1
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Ross AJ, Krumova I, Tunc B, Wu Q, Wu C, Camelliti P. A novel method to extend viability and functionality of living heart slices. Front Cardiovasc Med 2023; 10:1244630. [PMID: 37881724 PMCID: PMC10597746 DOI: 10.3389/fcvm.2023.1244630] [Citation(s) in RCA: 0] [Impact Index Per Article: 0] [Reference Citation Analysis] [Abstract] [Key Words] [Grants] [Track Full Text] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Received: 06/22/2023] [Accepted: 08/09/2023] [Indexed: 10/27/2023] Open
Abstract
Living heart slices have recently emerged as a powerful experimental model for fundamental cardiac research. By retaining the structure and function of the native myocardium while maintaining the simplicity of cell culture models, heart slices can be easily employed in electrophysiological, pharmacological, biochemical, and structural investigations. One single heart yields many slices (>20 slices for rodents, >100 slices for porcine or human hearts), however due to the low throughput of most assays and rapid slice degeneration within 24 h of preparation, many slices remain unused and are discarded at the end of the preparation day. Here we present a novel method to extend viability and functionality of living heart slices, enabling their use in experiments over several consecutive days following preparation. By combining hypothermic conditions with inhibition of myosin II ATPase using 2,3-butanedione monoxime (BDM), slices prepared from the left ventricle of porcine hearts remain viable and exhibit preserved contractile function and morphology for up to 6 days. Electrophysiological function was also confirmed over the 6 days by extracellular field potentials recordings. This simple method not only maximizes the use of slices prepared from one single heart, thus reducing the number of animals required, but also increases data reproducibility by allowing multiple electrophysiological, pharmacological, biochemical, and structural studies to be performed from the same heart.
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Affiliation(s)
- Abigail J. Ross
- School of Biosciences and Medicine, University of Surrey, Guildford, United Kingdom
| | - Iva Krumova
- School of Biosciences and Medicine, University of Surrey, Guildford, United Kingdom
| | - Berfin Tunc
- School of Biosciences and Medicine, University of Surrey, Guildford, United Kingdom
| | - Qin Wu
- School of Biosciences and Medicine, University of Surrey, Guildford, United Kingdom
- School of Medicine, Jiangsu Vocational College of Medicine, Yancheng, China
| | - Changhao Wu
- School of Biosciences and Medicine, University of Surrey, Guildford, United Kingdom
| | - Patrizia Camelliti
- School of Biosciences and Medicine, University of Surrey, Guildford, United Kingdom
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2
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Li J, Sundnes J, Hou Y, Laasmaa M, Ruud M, Unger A, Kolstad TR, Frisk M, Norseng PA, Yang L, Setterberg IE, Alves ES, Kalakoutis M, Sejersted OM, Lanner JT, Linke WA, Lunde IG, de Tombe PP, Louch WE. Stretch Harmonizes Sarcomere Strain Across the Cardiomyocyte. Circ Res 2023; 133:255-270. [PMID: 37401464 PMCID: PMC10355805 DOI: 10.1161/circresaha.123.322588] [Citation(s) in RCA: 0] [Impact Index Per Article: 0] [Reference Citation Analysis] [Abstract] [Key Words] [MESH Headings] [Track Full Text] [Journal Information] [Submit a Manuscript] [Subscribe] [Scholar Register] [Received: 01/27/2023] [Revised: 06/07/2023] [Accepted: 06/22/2023] [Indexed: 07/05/2023]
Abstract
BACKGROUND Increasing cardiomyocyte contraction during myocardial stretch serves as the basis for the Frank-Starling mechanism in the heart. However, it remains unclear how this phenomenon occurs regionally within cardiomyocytes, at the level of individual sarcomeres. We investigated sarcomere contractile synchrony and how intersarcomere dynamics contribute to increasing contractility during cell lengthening. METHODS Sarcomere strain and Ca2+ were simultaneously recorded in isolated left ventricular cardiomyocytes during 1 Hz field stimulation at 37 °C, at resting length and following stepwise stretch. RESULTS We observed that in unstretched rat cardiomyocytes, differential sarcomere deformation occurred during each beat. Specifically, while most sarcomeres shortened during the stimulus, ≈10% to 20% of sarcomeres were stretched or remained stationary. This nonuniform strain was not traced to regional Ca2+ disparities but rather shorter resting lengths and lower force production in systolically stretched sarcomeres. Lengthening of the cell recruited additional shortening sarcomeres, which increased contractile efficiency as less negative, wasted work was performed by stretched sarcomeres. Given the known role of titin in setting sarcomere dimensions, we next hypothesized that modulating titin expression would alter intersarcomere dynamics. Indeed, in cardiomyocytes from mice with titin haploinsufficiency, we observed greater variability in resting sarcomere length, lower recruitment of shortening sarcomeres, and impaired work performance during cell lengthening. CONCLUSIONS Graded sarcomere recruitment directs cardiomyocyte work performance, and harmonization of sarcomere strain increases contractility during cell stretch. By setting sarcomere dimensions, titin controls sarcomere recruitment, and its lowered expression in haploinsufficiency mutations impairs cardiomyocyte contractility.
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Affiliation(s)
- Jia Li
- Institute for Experimental Medical Research, Oslo University Hospital and University of Oslo, Norway (J.L., Y.H., M.L., M.R., T.R.K., M.F., P.A.N., I.E.S., O.M.S., I.G.L., W.E.L.)
- KG Jebsen Center for Cardiac Research, University of Oslo, Norway (J.L., Y.H., M.L., M.R., T.R.K., M.F., I.E.S., O.M.S., I.G.L., W.E.L.)
| | | | - Yufeng Hou
- Institute for Experimental Medical Research, Oslo University Hospital and University of Oslo, Norway (J.L., Y.H., M.L., M.R., T.R.K., M.F., P.A.N., I.E.S., O.M.S., I.G.L., W.E.L.)
- KG Jebsen Center for Cardiac Research, University of Oslo, Norway (J.L., Y.H., M.L., M.R., T.R.K., M.F., I.E.S., O.M.S., I.G.L., W.E.L.)
| | - Martin Laasmaa
- Institute for Experimental Medical Research, Oslo University Hospital and University of Oslo, Norway (J.L., Y.H., M.L., M.R., T.R.K., M.F., P.A.N., I.E.S., O.M.S., I.G.L., W.E.L.)
- KG Jebsen Center for Cardiac Research, University of Oslo, Norway (J.L., Y.H., M.L., M.R., T.R.K., M.F., I.E.S., O.M.S., I.G.L., W.E.L.)
| | - Marianne Ruud
- Institute for Experimental Medical Research, Oslo University Hospital and University of Oslo, Norway (J.L., Y.H., M.L., M.R., T.R.K., M.F., P.A.N., I.E.S., O.M.S., I.G.L., W.E.L.)
- KG Jebsen Center for Cardiac Research, University of Oslo, Norway (J.L., Y.H., M.L., M.R., T.R.K., M.F., I.E.S., O.M.S., I.G.L., W.E.L.)
| | - Andreas Unger
- Institute of Physiology II, University of Münster, Germany (A.U., W.A.L.)
| | - Terje R. Kolstad
- Institute for Experimental Medical Research, Oslo University Hospital and University of Oslo, Norway (J.L., Y.H., M.L., M.R., T.R.K., M.F., P.A.N., I.E.S., O.M.S., I.G.L., W.E.L.)
- KG Jebsen Center for Cardiac Research, University of Oslo, Norway (J.L., Y.H., M.L., M.R., T.R.K., M.F., I.E.S., O.M.S., I.G.L., W.E.L.)
| | - Michael Frisk
- Institute for Experimental Medical Research, Oslo University Hospital and University of Oslo, Norway (J.L., Y.H., M.L., M.R., T.R.K., M.F., P.A.N., I.E.S., O.M.S., I.G.L., W.E.L.)
- KG Jebsen Center for Cardiac Research, University of Oslo, Norway (J.L., Y.H., M.L., M.R., T.R.K., M.F., I.E.S., O.M.S., I.G.L., W.E.L.)
| | - Per Andreas Norseng
- Institute for Experimental Medical Research, Oslo University Hospital and University of Oslo, Norway (J.L., Y.H., M.L., M.R., T.R.K., M.F., P.A.N., I.E.S., O.M.S., I.G.L., W.E.L.)
| | | | - Ingunn E. Setterberg
- Institute for Experimental Medical Research, Oslo University Hospital and University of Oslo, Norway (J.L., Y.H., M.L., M.R., T.R.K., M.F., P.A.N., I.E.S., O.M.S., I.G.L., W.E.L.)
- KG Jebsen Center for Cardiac Research, University of Oslo, Norway (J.L., Y.H., M.L., M.R., T.R.K., M.F., I.E.S., O.M.S., I.G.L., W.E.L.)
| | - Estela S. Alves
- Department of Physiology and Pharmacology, Karolinska Institutet, Stockholm, Sweden (E.S.A., M.K., J.T.L.)
| | - Michaeljohn Kalakoutis
- Department of Physiology and Pharmacology, Karolinska Institutet, Stockholm, Sweden (E.S.A., M.K., J.T.L.)
| | - Ole M. Sejersted
- Institute for Experimental Medical Research, Oslo University Hospital and University of Oslo, Norway (J.L., Y.H., M.L., M.R., T.R.K., M.F., P.A.N., I.E.S., O.M.S., I.G.L., W.E.L.)
- KG Jebsen Center for Cardiac Research, University of Oslo, Norway (J.L., Y.H., M.L., M.R., T.R.K., M.F., I.E.S., O.M.S., I.G.L., W.E.L.)
| | - Johanna T. Lanner
- Department of Physiology and Pharmacology, Karolinska Institutet, Stockholm, Sweden (E.S.A., M.K., J.T.L.)
| | - Wolfgang A. Linke
- Institute of Physiology II, University of Münster, Germany (A.U., W.A.L.)
| | - Ida G. Lunde
- Institute for Experimental Medical Research, Oslo University Hospital and University of Oslo, Norway (J.L., Y.H., M.L., M.R., T.R.K., M.F., P.A.N., I.E.S., O.M.S., I.G.L., W.E.L.)
- KG Jebsen Center for Cardiac Research, University of Oslo, Norway (J.L., Y.H., M.L., M.R., T.R.K., M.F., I.E.S., O.M.S., I.G.L., W.E.L.)
| | - Pieter P. de Tombe
- Department of Physiology and Biophysics, University of Illinois at Chicago (P.P.d.T.)
- Phymedexp, Université de Montpellier, INSERM, CNRS, France (P.P.d.T.)
| | - William E. Louch
- Institute for Experimental Medical Research, Oslo University Hospital and University of Oslo, Norway (J.L., Y.H., M.L., M.R., T.R.K., M.F., P.A.N., I.E.S., O.M.S., I.G.L., W.E.L.)
- KG Jebsen Center for Cardiac Research, University of Oslo, Norway (J.L., Y.H., M.L., M.R., T.R.K., M.F., I.E.S., O.M.S., I.G.L., W.E.L.)
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3
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Lookin O, de Tombe P, Boulali N, Gergely C, Cloitre T, Cazorla O. Cardiomyocyte sarcomere length variability: Membrane fluorescence versus second harmonic generation myosin imaging. J Gen Physiol 2023; 155:213827. [PMID: 36695814 PMCID: PMC9930136 DOI: 10.1085/jgp.202213289] [Citation(s) in RCA: 0] [Impact Index Per Article: 0] [Reference Citation Analysis] [Abstract] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Received: 10/27/2022] [Revised: 12/07/2022] [Accepted: 01/10/2023] [Indexed: 01/26/2023] Open
Abstract
Sarcomere length (SL) and its variation along the myofibril strongly regulate integrated coordinated myocyte contraction. It is therefore important to obtain individual SL properties. Optical imaging by confocal fluorescence (for example, using ANEPPS) or transmitted light microscopy is often used for this purpose. However, this allows for the visualization of structures related to Z-disks only. In contrast, second-harmonic generation (SHG) microscopy visualizes A-band sarcomeric structures directly. Here, we compared averaged SL and its variability in isolated relaxed rat cardiomyocytes by imaging with ANEPPS and SHG. We found that SL variability, evaluated by several absolute and relative measures, is two times smaller using SHG vs. ANEPPS, while both optical methods give the same average (median) SL. We conclude that optical methods with similar optical spatial resolution provide valid estimations of average SL, but the use of SHG microscopy for visualization of sarcomeric A-bands may be the "gold standard" for evaluation of SL variability due to the absence of optical interference between the sarcomere center and non-sarcomeric structures. This contrasts with sarcomere edges where t-tubules may not consistently colocalize to Z-disks. The use of SHG microscopy instead of fluorescent imaging can be a prospective tool to map sarcomere variability both in vitro and in vivo conditions and to reveal its role in the functional behavior of living myocardium.
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Affiliation(s)
- Oleg Lookin
- Institute of Immunology and Physiology , Ural Branch of Russian Academy of Sciences , Yekaterinburg, Russia
| | - Pieter de Tombe
- Laboratory "Physiologie et Médecine Expérimentale du Coeur et des Muscles", Phymedexp, INSERM, CNRS, Montpellier University , Montpellier, France.,Physiology and Biophysics, University of Illinois at Chicago , Chicago, IL, USA
| | - Najlae Boulali
- Laboratory "Physiologie et Médecine Expérimentale du Coeur et des Muscles", Phymedexp, INSERM, CNRS, Montpellier University , Montpellier, France
| | - Csilla Gergely
- L2C, University of Montpellier , CNRS , Montpellier, France
| | | | - Olivier Cazorla
- Laboratory "Physiologie et Médecine Expérimentale du Coeur et des Muscles", Phymedexp, INSERM, CNRS, Montpellier University , Montpellier, France
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4
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Kohl P, Zgierski-Johnston CM. Assessment of Tissue Viability by Functional Imaging of Membrane Potential. Methods Mol Biol 2023; 2644:423-434. [PMID: 37142938 DOI: 10.1007/978-1-0716-3052-5_27] [Citation(s) in RCA: 0] [Impact Index Per Article: 0] [Reference Citation Analysis] [Abstract] [Key Words] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Indexed: 05/06/2023]
Abstract
Electrical activity plays a key role in physiology, in particular for signaling and coordination. Cellular electrophysiology is often studied with micropipette-based techniques such as patch clamp and sharp electrodes, but for measurements at the tissue or organ scale, more integrated approaches are needed. Epifluorescence imaging of voltage-sensitive dyes ("optical mapping") is a tissue non-destructive approach to obtain insight into electrophysiology with high spatiotemporal resolution. Optical mapping has primarily been applied to excitable organs, especially the heart and brain. Action potential durations, conduction patterns, and conduction velocities can be determined from the recordings, providing information about electrophysiological mechanisms, including factors such as effects of pharmacological interventions, ion channel mutations, or tissue remodeling. Here, we describe the process for optical mapping of Langendorff-perfused mouse hearts, highlighting potential issues and key considerations.
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Affiliation(s)
- Peter Kohl
- Institute for Experimental Cardiovascular Medicine, University Heart Center Freiburg-Bad Krozingen, Freiburg im Breisgau, Germany
- Faculty of Medicine, University of Freiburg, Freiburg im Breisgau, Germany
| | - Callum M Zgierski-Johnston
- Institute for Experimental Cardiovascular Medicine, University Heart Center Freiburg-Bad Krozingen, Freiburg im Breisgau, Germany.
- Faculty of Medicine, University of Freiburg, Freiburg im Breisgau, Germany.
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5
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Kuo CW, Pratiwi FW, Liu YT, Chueh DY, Chen P. Revealing the nanometric structural changes in myocardial infarction models by time-lapse intravital imaging. Front Bioeng Biotechnol 2022; 10:935415. [PMID: 36051583 PMCID: PMC9424828 DOI: 10.3389/fbioe.2022.935415] [Citation(s) in RCA: 0] [Impact Index Per Article: 0] [Reference Citation Analysis] [Abstract] [Track Full Text] [Download PDF] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Received: 05/05/2022] [Accepted: 07/25/2022] [Indexed: 11/13/2022] Open
Abstract
In the development of bioinspired nanomaterials for therapeutic applications, it is very important to validate the design of nanomaterials in the disease models. Therefore, it is desirable to visualize the change of the cells in the diseased site at the nanoscale. Heart diseases often start with structural, morphological, and functional alterations of cardiomyocyte components at the subcellular level. Here, we developed straightforward technique for long-term real-time intravital imaging of contracting hearts without the need of cardiac pacing and complex post processing images to understand the subcellular structural and dynamic changes in the myocardial infarction model. A two-photon microscope synchronized with electrocardiogram signals was used for long-term in vivo imaging of a contracting heart with subcellular resolution. We found that the structural and dynamic behaviors of organelles in cardiomyocytes closely correlated with heart function. In the myocardial infarction model, sarcomere shortening decreased from ∼15% (healthy) to ∼8% (diseased) as a result of impaired cardiac function, whereas the distances between sarcomeres increased by 100 nm (from 2.11 to 2.21 μm) in the diastolic state. In addition, T-tubule system regularity analysis revealed that T-tubule structures that were initially highly organized underwent significant remodeling. Morphological remodeling and changes in dynamic activity at the subcellular level are essential to maintain heart function after infarction in a heart disease model.
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Affiliation(s)
- Chiung Wen Kuo
- Research Center for Applied Science, Academia Sinica, Taipei, Taiwan
| | | | - Yen-Ting Liu
- Research Center for Applied Science, Academia Sinica, Taipei, Taiwan
| | - Di-Yen Chueh
- Research Center for Applied Science, Academia Sinica, Taipei, Taiwan
| | - Peilin Chen
- Research Center for Applied Science, Academia Sinica, Taipei, Taiwan
- Institute of Physics, Academia Sinica, Taipei, Taiwan
- *Correspondence: Peilin Chen,
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6
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Helmes M, Palmer BM. Sarcomere length in the beating heart: Synchronicity is optional. J Gen Physiol 2022; 154:212954. [PMID: 35015810 PMCID: PMC8756987 DOI: 10.1085/jgp.202113022] [Citation(s) in RCA: 0] [Impact Index Per Article: 0] [Reference Citation Analysis] [Abstract] [Track Full Text] [Download PDF] [Journal Information] [Subscribe] [Scholar Register] [Indexed: 11/20/2022] Open
Abstract
Helmes and Palmer review research by Kobirumaki-Shimozawa et al.
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Affiliation(s)
- Michiel Helmes
- Department of Physiology, Amsterdam University Medical Centre, Amsterdam, Netherlands
| | - Bradley M Palmer
- Department of Molecular Physiology and Biophysics, University of Vermont, Burlington, VT
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7
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Giardini F, Lazzeri E, Vitale G, Ferrantini C, Costantini I, Pavone FS, Poggesi C, Bocchi L, Sacconi L. Quantification of Myocyte Disarray in Human Cardiac Tissue. Front Physiol 2021; 12:750364. [PMID: 34867455 PMCID: PMC8635020 DOI: 10.3389/fphys.2021.750364] [Citation(s) in RCA: 1] [Impact Index Per Article: 0.3] [Reference Citation Analysis] [Abstract] [Key Words] [Track Full Text] [Download PDF] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Received: 07/30/2021] [Accepted: 09/24/2021] [Indexed: 11/13/2022] Open
Abstract
Proper three-dimensional (3D)-cardiomyocyte orientation is important for an effective tension production in cardiac muscle. Cardiac diseases can cause severe remodeling processes in the heart, such as cellular misalignment, that can affect both the electrical and mechanical functions of the organ. To date, a proven methodology to map and quantify myocytes disarray in massive samples is missing. In this study, we present an experimental pipeline to reconstruct and analyze the 3D cardiomyocyte architecture in massive samples. We employed tissue clearing, staining, and advanced microscopy techniques to detect sarcomeres in relatively large human myocardial strips with micrometric resolution. Z-bands periodicity was exploited in a frequency analysis approach to extract the 3D myofilament orientation, providing an orientation map used to characterize the tissue organization at different spatial scales. As a proof-of-principle, we applied the proposed method to healthy and pathologically remodeled human cardiac tissue strips. Preliminary results suggest the reliability of the method: strips from a healthy donor are characterized by a well-organized tissue, where the local disarray is log-normally distributed and slightly depends on the spatial scale of analysis; on the contrary, pathological strips show pronounced tissue disorganization, characterized by local disarray significantly dependent on the spatial scale of analysis. A virtual sample generator is developed to link this multi-scale disarray analysis with the underlying cellular architecture. This approach allowed us to quantitatively assess tissue organization in terms of 3D myocyte angular dispersion and may pave the way for developing novel predictive models based on structural data at cellular resolution.
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Affiliation(s)
- Francesco Giardini
- Laboratory of Non-Linear Spectroscopy (LENS), University of Florence, Sesto Fiorentino, Italy
| | - Erica Lazzeri
- Laboratory of Non-Linear Spectroscopy (LENS), University of Florence, Sesto Fiorentino, Italy
| | - Giulia Vitale
- Division of Physiology, Department of Clinical and Experimental Medicine, University of Florence, Florence, Italy
| | - Cecilia Ferrantini
- Laboratory of Non-Linear Spectroscopy (LENS), University of Florence, Sesto Fiorentino, Italy.,Division of Physiology, Department of Clinical and Experimental Medicine, University of Florence, Florence, Italy
| | - Irene Costantini
- Laboratory of Non-Linear Spectroscopy (LENS), University of Florence, Sesto Fiorentino, Italy.,National Institute of Optics, National Research Council, University of Florence, Florence, Italy.,Department of Biology, University of Florence, Florence, Italy
| | - Francesco S Pavone
- Laboratory of Non-Linear Spectroscopy (LENS), University of Florence, Sesto Fiorentino, Italy.,National Institute of Optics, National Research Council, University of Florence, Florence, Italy.,Department of Physics, University of Florence, Florence, Italy
| | - Corrado Poggesi
- Division of Physiology, Department of Clinical and Experimental Medicine, University of Florence, Florence, Italy
| | - Leonardo Bocchi
- Laboratory of Non-Linear Spectroscopy (LENS), University of Florence, Sesto Fiorentino, Italy.,Department of Information Engineering, University of Florence, Florence, Italy
| | - Leonardo Sacconi
- Laboratory of Non-Linear Spectroscopy (LENS), University of Florence, Sesto Fiorentino, Italy.,National Institute of Optics, National Research Council, University of Florence, Florence, Italy.,Faculty of Medicine, Institute for Experimental Cardiovascular Medicine, University of Freiburg, Freiburg im Breisgau, Germany
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8
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Kobirumaki-Shimozawa F, Shimozawa T, Oyama K, Baba S, Li J, Nakanishi T, Terui T, Louch WE, Ishiwata S, Fukuda N. Synchrony of sarcomeric movement regulates left ventricular pump function in the in vivo beating mouse heart. J Gen Physiol 2021; 153:212675. [PMID: 34605861 PMCID: PMC8493835 DOI: 10.1085/jgp.202012860] [Citation(s) in RCA: 10] [Impact Index Per Article: 3.3] [Reference Citation Analysis] [Abstract] [Track Full Text] [Download PDF] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Received: 01/14/2021] [Accepted: 09/03/2021] [Indexed: 11/20/2022] Open
Abstract
Sarcomeric contraction in cardiomyocytes serves as the basis for the heart's pump functions. It has generally been considered that in cardiac muscle as well as in skeletal muscle, sarcomeres equally contribute to myofibrillar dynamics in myocytes at varying loads by producing similar levels of active and passive force. In the present study, we expressed α-actinin-AcGFP in Z-disks to analyze dynamic behaviors of sequentially connected individual sarcomeres along a myofibril in a left ventricular (LV) myocyte of the in vivo beating mouse heart. To quantify the magnitude of the contribution of individual sarcomeres to myofibrillar dynamics, we introduced the novel parameter "contribution index" (CI) to measure the synchrony in movements between a sarcomere and a myofibril (from -1 [complete asynchrony] to 1 [complete synchrony]). First, CI varied markedly between sarcomeres, with an average value of ∼0.3 during normal systole. Second, when the movements between adjacent sarcomeres were asynchronous (CI < 0), a sarcomere and the ones next to the adjacent sarcomeres and farther away moved in synchrony (CI > 0) along a myofibril. Third, when difference in LV pressure in diastole and systole (ΔLVP) was lowered to <10 mm Hg, diastolic sarcomere length increased. Under depressed conditions, the movements between adjacent sarcomeres were in marked asynchrony (CI, -0.3 to -0.4), and, as a result, average CI was linearly decreased in association with a decrease in ΔLVP. These findings suggest that in the left ventricle of the in vivo beating mouse heart, (1) sarcomeres heterogeneously contribute to myofibrillar dynamics due to an imbalance of active and passive force between neighboring sarcomeres, (2) the force imbalance is pronounced under depressed conditions coupled with a marked increase in passive force and the ensuing tug-of-war between sarcomeres, and (3) sarcomere synchrony via the distal intersarcomere interaction regulates the heart's pump function in coordination with myofibrillar contractility.
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Affiliation(s)
| | - Togo Shimozawa
- Technical Division, School of Science, The University of Tokyo, Tokyo, Japan
| | - Kotaro Oyama
- Department of Cell Physiology, The Jikei University School of Medicine, Tokyo, Japan.,Quantum Beam Science Research Directorate, National Institutes for Quantum and Radiological Science and Technology, Gunma, Japan
| | - Shunsuke Baba
- Department of Pediatrics, The Jikei University School of Medicine, Tokyo, Japan
| | - Jia Li
- Institute for Experimental Medical Research, Oslo University Hospital and University of Oslo, Oslo, Norway
| | - Tomohiro Nakanishi
- Department of Cell Physiology, The Jikei University School of Medicine, Tokyo, Japan
| | - Takako Terui
- Department of Anesthesiology, The Jikei University School of Medicine, Tokyo, Japan
| | - William E Louch
- Institute for Experimental Medical Research, Oslo University Hospital and University of Oslo, Oslo, Norway.,K.G. Jebsen Center for Cardiac Research, University of Oslo, Oslo, Norway
| | - Shin'ichi Ishiwata
- Department of Physics, Faculty of Science and Engineering, Waseda University, Tokyo, Japan
| | - Norio Fukuda
- Department of Cell Physiology, The Jikei University School of Medicine, Tokyo, Japan
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9
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Kitsara M, Tassis G, Papagiannopoulos A, Simon A, Agbulut O, Pispas S. Polysaccharide-Protein Multilayers Based on Chitosan-Fibrinogen Assemblies for Cardiac Cell Engineering. Macromol Biosci 2021; 22:e2100346. [PMID: 34648684 DOI: 10.1002/mabi.202100346] [Citation(s) in RCA: 3] [Impact Index Per Article: 1.0] [Reference Citation Analysis] [Abstract] [Key Words] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Received: 08/27/2021] [Revised: 10/10/2021] [Indexed: 12/11/2022]
Abstract
The cell and tissue culture substrates play a pivotal role in the regulation of cell-matrix and cell-cell interactions. The surface properties of the materials control a wide variety of cell functions. Amongst various methods, layer-by-layer (LbL) assembly is a versatile surface coating technique for creating controllable bio-coatings. Here, polysaccharide/protein multilayers are proposed, which are fabricated by immersive LbL assembly and based on the chitosan/fibrinogen pair for improving the adhesion and spreading of cardiomyocytes. Two approaches in LbL assembly are employed for clarifying the effect of the bilayers order and their concentration on cardiomyocytes viability and morphology. Fourier transform infrared spectroscopy (FTIR) measurements show that the adsorption of the biopolymers is enhanced during the LbL deposition in a synergistic manner. Contact angle measurements indicate that the multilayers are alternating from less to more hydrophilic behavior depending on the biopolymer that is added last. Confocal microscopy with immunostained fibrinogen reveals that the amount of the protein is higher when the concentration of the immersion solution is increased, however, for low solution concentration it is speculated that interdigitation between the separate biopolymer layers takes place. This work motivates the use of fibrinogen in polysaccharide/protein multilayers for enhanced cytocompatibility in cardiac tissue engineering.
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Affiliation(s)
- Maria Kitsara
- Institut de Biologie Paris-Seine, CNRS UMR 8256, INSERM ERL 1164, Biological Adaptation and Ageing, Sorbonne Université, Paris, 75005, France
| | - George Tassis
- Theoretical and Physical Chemistry Institute, National Hellenic Research Foundation, 48 Vassileos Constantinou Avenue, Athens, 11635, Greece.,Department of Physics, University of Patras, Patras, 26504, Greece
| | - Aristeidis Papagiannopoulos
- Theoretical and Physical Chemistry Institute, National Hellenic Research Foundation, 48 Vassileos Constantinou Avenue, Athens, 11635, Greece
| | - Alexandre Simon
- Institut de Biologie Paris-Seine, CNRS UMR 8256, INSERM ERL 1164, Biological Adaptation and Ageing, Sorbonne Université, Paris, 75005, France
| | - Onnik Agbulut
- Institut de Biologie Paris-Seine, CNRS UMR 8256, INSERM ERL 1164, Biological Adaptation and Ageing, Sorbonne Université, Paris, 75005, France
| | - Stergios Pispas
- Theoretical and Physical Chemistry Institute, National Hellenic Research Foundation, 48 Vassileos Constantinou Avenue, Athens, 11635, Greece
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10
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Boldt K, Joumaa V, MacDonald G, Rios JL, Herzog W. Cardiac ventricular muscle mechanical properties through the first year of life in Sprague-Dawley rats. Mech Ageing Dev 2020; 192:111359. [PMID: 32956701 DOI: 10.1016/j.mad.2020.111359] [Citation(s) in RCA: 0] [Impact Index Per Article: 0] [Reference Citation Analysis] [Abstract] [Key Words] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Received: 06/16/2020] [Revised: 08/20/2020] [Accepted: 09/14/2020] [Indexed: 10/23/2022]
Abstract
Advanced age has been shown to result in decreased compliance, shortening velocity, and calcium sensitivity of the heart muscle. Even though cardiac health has been studied extensively in elderly populations, relatively little is known about cardiac health and age for the first part of adulthood. The purpose of this study was to compare cardiac contractile properties across the first year of life in rats (between 17-53 weeks), corresponding to early to mid-adulthood. Hearts were harvested from rats aged 17-, 24-, 36-, and 53-weeks. Skinned cardiac trabecular fibre bundle testing was used to evaluate active and passive force properties, maximum shortening velocity, calcium sensitivity, and myosin heavy chain isoforms. Maximum active stress production was not different between age groups. Calcium sensitivity increased progressively, while shortening velocity remained unchanged after an increase from 17-and 24-weeks. Passive stiffness decreased between 17- and 24-weeks, but then increased progressively through to 53-weeks. Thus, many of the observed detrimental changes in systolic function (reduced shortening velocity and calcium sensitivity) associated with aging, do not seem to occur in early to mid-adulthood, while early signs of increased diastolic stiffness manifest within 53 weeks of age and may represent a first sign of decreasing heart function and health.
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Affiliation(s)
- Kevin Boldt
- Human Performance Laboratory, Faculty of Kinesiology, University of Calgary, Calgary, AB, Canada.
| | - Venus Joumaa
- Human Performance Laboratory, Faculty of Kinesiology, University of Calgary, Calgary, AB, Canada
| | - Graham MacDonald
- Human Performance Laboratory, Faculty of Kinesiology, University of Calgary, Calgary, AB, Canada
| | - Jaqueline Lourdes Rios
- Human Performance Laboratory, Faculty of Kinesiology, University of Calgary, Calgary, AB, Canada
| | - Walter Herzog
- Human Performance Laboratory, Faculty of Kinesiology, University of Calgary, Calgary, AB, Canada; Biomechanics Laboratory, School of Sports, Federal University of Santa Catarina, Florianopolis, SC, Brazil
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11
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Allen ME, Pennington ER, Perry JB, Dadoo S, Makrecka-Kuka M, Dambrova M, Moukdar F, Patel HD, Han X, Kidd GK, Benson EK, Raisch TB, Poelzing S, Brown DA, Shaikh SR. The cardiolipin-binding peptide elamipretide mitigates fragmentation of cristae networks following cardiac ischemia reperfusion in rats. Commun Biol 2020; 3:389. [PMID: 32680996 PMCID: PMC7368046 DOI: 10.1038/s42003-020-1101-3] [Citation(s) in RCA: 25] [Impact Index Per Article: 6.3] [Reference Citation Analysis] [Abstract] [Key Words] [MESH Headings] [Grants] [Track Full Text] [Download PDF] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Received: 05/23/2019] [Accepted: 06/23/2020] [Indexed: 01/05/2023] Open
Abstract
Mitochondrial dysfunction contributes to cardiac pathologies. Barriers to new therapies include an incomplete understanding of underlying molecular culprits and a lack of effective mitochondria-targeted medicines. Here, we test the hypothesis that the cardiolipin-binding peptide elamipretide, a clinical-stage compound under investigation for diseases of mitochondrial dysfunction, mitigates impairments in mitochondrial structure-function observed after rat cardiac ischemia-reperfusion. Respirometry with permeabilized ventricular fibers indicates that ischemia-reperfusion induced decrements in the activity of complexes I, II, and IV are alleviated with elamipretide. Serial block face scanning electron microscopy used to create 3D reconstructions of cristae ultrastructure reveals that disease-induced fragmentation of cristae networks are improved with elamipretide. Mass spectrometry shows elamipretide did not protect against the reduction of cardiolipin concentration after ischemia-reperfusion. Finally, elamipretide improves biophysical properties of biomimetic membranes by aggregating cardiolipin. The data suggest mitochondrial structure-function are interdependent and demonstrate elamipretide targets mitochondrial membranes to sustain cristae networks and improve bioenergetic function.
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Affiliation(s)
- Mitchell E Allen
- Department of Human Nutrition, Foods, and Exercise, Virginia Tech, Blacksburg, VA, USA
| | - Edward Ross Pennington
- Department of Biochemistry and Molecular Biology, East Carolina University, Greenville, NC, USA
- Department of Nutrition, Gillings School of Global Public Health and School of Medicine, University of North Carolina at Chapel Hill, Chapel Hill, NC, USA
| | - Justin B Perry
- Department of Human Nutrition, Foods, and Exercise, Virginia Tech, Blacksburg, VA, USA
| | - Sahil Dadoo
- Department of Nutrition, Gillings School of Global Public Health and School of Medicine, University of North Carolina at Chapel Hill, Chapel Hill, NC, USA
| | | | - Maija Dambrova
- Latvian Institute for Organic Synthesis Riga Latvia, Norwich, UK
| | - Fatiha Moukdar
- Department of Physiology, East Carolina University, Greenville, NC, USA
| | - Hetal D Patel
- Department of Physiology, East Carolina University, Greenville, NC, USA
| | - Xianlin Han
- Barshop Institute for Longevity and Aging Studies, University of Texas Health Science Center, San Antonio, TX, USA
| | - Grahame K Kidd
- Department of Neurosciences, Cleveland Clinic, Cleveland, OH, USA
- Renovo Neural Inc, Cleveland, OH, USA
| | | | - Tristan B Raisch
- Virginia Tech Faculty of Health Sciences, Roanoke, VA, USA
- Fralin Biomedical Research Institute at Virginia Tech Carillion, Roanoke, VA, USA
| | - Steven Poelzing
- Virginia Tech Faculty of Health Sciences, Roanoke, VA, USA
- Fralin Biomedical Research Institute at Virginia Tech Carillion, Roanoke, VA, USA
- Translational Biology, Medicine and Health, Virginia Tech, Roanoke, VA, USA
- Department of Biomedical Engineering and Mechanics, Virginia Tech, Blacksburg, VA, USA
| | - David A Brown
- Department of Human Nutrition, Foods, and Exercise, Virginia Tech, Blacksburg, VA, USA
- Virginia Tech Faculty of Health Sciences, Roanoke, VA, USA
- Virginia Tech Center for Drug Discovery, Blacksburg, VA, USA
- Virginia Tech Metabolism Core Virginia Tech, Blacksburg, VA, USA
| | - Saame Raza Shaikh
- Department of Nutrition, Gillings School of Global Public Health and School of Medicine, University of North Carolina at Chapel Hill, Chapel Hill, NC, USA.
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12
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Andrei SR, Ghosh M, Sinharoy P, Damron DS. Stimulation of TRPA1 attenuates ischemia-induced cardiomyocyte cell death through an eNOS-mediated mechanism. Channels (Austin) 2020; 13:192-206. [PMID: 31161862 PMCID: PMC6557600 DOI: 10.1080/19336950.2019.1623591] [Citation(s) in RCA: 11] [Impact Index Per Article: 2.8] [Reference Citation Analysis] [Abstract] [Key Words] [Track Full Text] [Download PDF] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Indexed: 12/22/2022] Open
Abstract
The functional expression of transient receptor potential cation channel of the ankyrin-1 subtype (TRPA1) has recently been identified in adult mouse cardiac tissue where stimulation of this ion channel leads to increases in adult mouse ventricular cardiomyocyte (CM) contractile function via a Ca2+-Calmodulin-dependent kinase (CaMKII) pathway. However, the extent to which TRPA1 induces nitric oxide (NO) production in CMs, and whether this signaling cascade mediates physiological or pathophysiological events in cardiac tissue remains elusive. Freshly isolated CMs from wild-type (WT) or TRPA1 knockout (TRPA1-/-) mouse hearts were treated with AITC (100 µM) and prepared for immunoblot, NO detection or ischemia protocols. Our findings demonstrate that TRPA1 stimulation with AITC results in phosphorylation of protein kinase B (Akt) and endothelial NOS (eNOS) concomitantly with NO production in a concentration- and time-dependent manner. Additionally, we found that TRPA1 induced increases in CM [Ca2+]i and contractility occur independently of Akt and eNOS activation mechanisms. Further analysis revealed that the presence and activation of TRPA1 promotes CM survival and viability following ischemic insult via a mechanism partially dependent upon eNOS. Therefore, activation of the TRPA1/Akt/eNOS pathway attenuates ischemia-induced CM cell death.
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Affiliation(s)
- Spencer R Andrei
- a Department of Medicine , Vanderbilt University Medical Center , Nashville , TN , USA
| | - Monica Ghosh
- b Department of Biomedical Sciences , Kent State University , Kent , OH , USA
| | - Pritam Sinharoy
- c Department of Biopharmaceutical Development , Medimmune LLC , Gaithersburg , MD , USA
| | - Derek S Damron
- b Department of Biomedical Sciences , Kent State University , Kent , OH , USA
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13
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Myachina TA, Butova KA, Lookin ON. Development and Program Implementation of an Algorithm to Estimate the Mean Sarcomere Length of a Cardiomyocyte. Biophysics (Nagoya-shi) 2019. [DOI: 10.1134/s0006350919050178] [Citation(s) in RCA: 6] [Impact Index Per Article: 1.2] [Reference Citation Analysis] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Indexed: 11/23/2022] Open
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14
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Kavanagh DPJ, Kalia N. Live Intravital Imaging of Cellular Trafficking in the Cardiac Microvasculature-Beating the Odds. Front Immunol 2019; 10:2782. [PMID: 31849965 PMCID: PMC6901937 DOI: 10.3389/fimmu.2019.02782] [Citation(s) in RCA: 1] [Impact Index Per Article: 0.2] [Reference Citation Analysis] [Abstract] [Key Words] [Track Full Text] [Download PDF] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Received: 08/21/2019] [Accepted: 11/13/2019] [Indexed: 12/11/2022] Open
Abstract
Although mortality rates from cardiovascular disease in the developed world are falling, the prevalence of cardiovascular disease (CVD) is not. Each year, the number of people either being diagnosed as suffering with CVD or undergoing a surgical procedure related to it, such as percutaneous coronary intervention, continues to increase. In order to ensure that we can effectively manage these diseases in the future, it is critical that we fully understand their basic physiology and their underlying causative factors. Over recent years, the important role of the cardiac microcirculation in both acute and chronic disorders of the heart has become clear. The recruitment of inflammatory cells into the cardiac microcirculation and their subsequent activation may contribute significantly to tissue damage, adverse remodeling, and poor outcomes during recovery. However, our basic understanding of the cardiac microcirculation is hampered by an historic inability to image the microvessels of the beating heart-something we have been able to achieve in other organs for over 100 years. This stems from a couple of clear and obvious difficulties related to imaging the heart-firstly, it has significant inherent contractile motion and is affected considerably by the movement of lungs. Secondly, it is located in an anatomically challenging position for microscopy. However, recent microscopic and technological developments have allowed us to overcome some of these challenges and to begin to answer some of the basic outstanding questions in cardiac microvascular physiology, particularly in relation to inflammatory cell recruitment. In this review, we will discuss some of the historic work that took place in the latter part of last century toward cardiac intravital, before moving onto the advanced work that has been performed since. This work, which has utilized technology such as spinning-disk confocal and multiphoton microscopy, has-along with some significant advancements in algorithms and software-unlocked our ability to image the "business end" of the cardiac vascular tree. This review will provide an overview of these techniques, as well as some practical pointers toward software and other tools that may be useful for other researchers who are considering utilizing this technique themselves.
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Affiliation(s)
- Dean Philip John Kavanagh
- Institute of Cardiovascular Sciences, College of Medical and Dental Sciences, University of Birmingham, Birmingham, United Kingdom
| | - Neena Kalia
- Institute of Cardiovascular Sciences, College of Medical and Dental Sciences, University of Birmingham, Birmingham, United Kingdom
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15
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Garcia-Canadilla P, Cook AC, Mohun TJ, Oji O, Schlossarek S, Carrier L, McKenna WJ, Moon JC, Captur G. Myoarchitectural disarray of hypertrophic cardiomyopathy begins pre-birth. J Anat 2019; 235:962-976. [PMID: 31347708 PMCID: PMC6794206 DOI: 10.1111/joa.13058] [Citation(s) in RCA: 27] [Impact Index Per Article: 5.4] [Reference Citation Analysis] [Abstract] [Key Words] [Track Full Text] [Download PDF] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Accepted: 06/17/2019] [Indexed: 01/24/2023] Open
Abstract
Myoarchitectural disarray – the multiscalar disorganisation of myocytes, is a recognised histopathological hallmark of adult human hypertrophic cardiomyopathy (HCM). It occurs before the establishment of left ventricular hypertrophy (LVH) but its early origins and evolution around the time of birth are unknown. Our aim is to investigate whether myoarchitectural abnormalities in HCM are present in the fetal heart. We used wild‐type, heterozygous and homozygous hearts (n = 56) from a Mybpc3‐targeted knock‐out HCM mouse model and imaged the 3D micro‐structure by high‐resolution episcopic microscopy. We developed a novel structure tensor approach to extract, display and quantify myocyte orientation and its local angular uniformity by helical angle, angle of intrusion and myoarchitectural disarray index, respectively, immediately before and after birth. In wild‐type, we demonstrate uniformity of orientation of cardiomyocytes with smooth transitions of helical angle transmurally both before and after birth but with traces of disarray at the septal insertion points of the right ventricle. In comparison, heterozygous mice free of LVH, and homozygous mice showed not only loss of the normal linear helical angulation transmural profiles observed in wild‐type but also fewer circumferentially arranged myocytes at birth. Heterozygous and homozygous showed more disarray with a wider distribution than in wild‐type before birth. In heterozygous mice, disarray was seen in the anterior, septal and inferior walls irrespective of stage, whereas in homozygous mice it extended to the whole LV circumference including the lateral wall. In conclusion, myoarchitectural disarray is detectable in the fetal heart of an HCM mouse model before the development of LVH.
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Affiliation(s)
| | - Andrew C Cook
- Institute of Cardiovascular Science, University College London, London, UK
| | | | - Onyedikachi Oji
- Institute of Cardiovascular Science, University College London, London, UK
| | - Saskia Schlossarek
- Cardiovascular Research Centre, Institute of Experimental Pharmacology and Toxicology, University Medical Center Hamburg-Eppendorf, Hamburg, Germany.,DZHK (German Center for Cardiovascular Research), partner site Hamburg/Kiel/Lübeck, Hamburg, Germany
| | - Lucie Carrier
- Cardiovascular Research Centre, Institute of Experimental Pharmacology and Toxicology, University Medical Center Hamburg-Eppendorf, Hamburg, Germany.,DZHK (German Center for Cardiovascular Research), partner site Hamburg/Kiel/Lübeck, Hamburg, Germany
| | - William J McKenna
- Institute of Cardiovascular Science, University College London, London, UK
| | - James C Moon
- Institute of Cardiovascular Science, University College London, London, UK.,The Cardiovascular Magnetic Resonance Imaging Unit, Barts Heart Centre, St Bartholomew's Hospital, London, UK
| | - Gabriella Captur
- Institute of Cardiovascular Science, University College London, London, UK
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16
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Toepfer CN, Sharma A, Cicconet M, Garfinkel AC, Mücke M, Neyazi M, Willcox JA, Agarwal R, Schmid M, Rao J, Ewoldt J, Pourquié O, Chopra A, Chen CS, Seidman JG, Seidman CE. SarcTrack. Circ Res 2019; 124:1172-1183. [PMID: 30700234 PMCID: PMC6485312 DOI: 10.1161/circresaha.118.314505] [Citation(s) in RCA: 76] [Impact Index Per Article: 15.2] [Reference Citation Analysis] [Abstract] [Key Words] [MESH Headings] [Grants] [Track Full Text] [Download PDF] [Figures] [Journal Information] [Submit a Manuscript] [Subscribe] [Scholar Register] [Received: 11/30/2018] [Revised: 01/18/2019] [Accepted: 01/30/2019] [Indexed: 12/18/2022]
Abstract
RATIONALE Human induced pluripotent stem cell-derived cardiomyocytes (hiPSC-CMs) in combination with CRISPR/Cas9 genome editing provide unparalleled opportunities to study cardiac biology and disease. However, sarcomeres, the fundamental units of myocyte contraction, are immature and nonlinear in hiPSC-CMs, which technically challenge accurate functional interrogation of contractile parameters in beating cells. Furthermore, existing analysis methods are relatively low-throughput, indirectly assess contractility, or only assess well-aligned sarcomeres found in mature cardiac tissues. OBJECTIVE We aimed to develop an analysis platform that directly, rapidly, and automatically tracks sarcomeres in beating cardiomyocytes. The platform should assess sarcomere content, contraction and relaxation parameters, and beat rate. METHODS AND RESULTS We developed SarcTrack, a MatLab software that monitors fluorescently tagged sarcomeres in hiPSC-CMs. The algorithm determines sarcomere content, sarcomere length, and returns rates of sarcomere contraction and relaxation. By rapid measurement of hundreds of sarcomeres in each hiPSC-CM, SarcTrack provides large data sets for robust statistical analyses of multiple contractile parameters. We validated SarcTrack by analyzing drug-treated hiPSC-CMs, confirming the contractility effects of compounds that directly activate (CK-1827452) or inhibit (MYK-461) myosin molecules or indirectly alter contractility (verapamil and propranolol). SarcTrack analysis of hiPSC-CMs carrying a heterozygous truncation variant in the myosin-binding protein C ( MYBPC3) gene, which causes hypertrophic cardiomyopathy, recapitulated seminal disease phenotypes including cardiac hypercontractility and diminished relaxation, abnormalities that normalized with MYK-461 treatment. CONCLUSIONS SarcTrack provides a direct and efficient method to quantitatively assess sarcomere function. By improving existing contractility analysis methods and overcoming technical challenges associated with functional evaluation of hiPSC-CMs, SarcTrack enhances translational prospects for sarcomere-regulating therapeutics and accelerates interrogation of human cardiac genetic variants.
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Affiliation(s)
- Christopher N. Toepfer
- From the Department of Genetics (C.N.T., A.S., A.C.G., M.N., J.A.L.W., R.A., M.S., J.R., O.P., J.G.S., C.E.S.), Harvard Medical School, Boston, MA
- Cardiovascular Medicine, Radcliffe Department of Medicine (C.N.T.), University of Oxford, United Kingdom
- Wellcome Centre for Human Genetics (C.N.T.), University of Oxford, United Kingdom
| | - Arun Sharma
- From the Department of Genetics (C.N.T., A.S., A.C.G., M.N., J.A.L.W., R.A., M.S., J.R., O.P., J.G.S., C.E.S.), Harvard Medical School, Boston, MA
| | - Marcelo Cicconet
- Image and Data Analysis Core (M.C.), Harvard Medical School, Boston, MA
| | - Amanda C. Garfinkel
- From the Department of Genetics (C.N.T., A.S., A.C.G., M.N., J.A.L.W., R.A., M.S., J.R., O.P., J.G.S., C.E.S.), Harvard Medical School, Boston, MA
| | - Michael Mücke
- Cardiovascular and Metabolic Sciences, Max Delbrück Center for Molecular Medicine, Berlin, Germany (M.M.)
- German Centre for Cardiovascular Research, Berlin, Germany (M.M.)
- Charité-Universitätsmedizin, Berlin, Germany (M.M.)
| | - Meraj Neyazi
- From the Department of Genetics (C.N.T., A.S., A.C.G., M.N., J.A.L.W., R.A., M.S., J.R., O.P., J.G.S., C.E.S.), Harvard Medical School, Boston, MA
- Hannover Medical School, Germany (M.N.)
| | - Jon A.L. Willcox
- From the Department of Genetics (C.N.T., A.S., A.C.G., M.N., J.A.L.W., R.A., M.S., J.R., O.P., J.G.S., C.E.S.), Harvard Medical School, Boston, MA
| | - Radhika Agarwal
- From the Department of Genetics (C.N.T., A.S., A.C.G., M.N., J.A.L.W., R.A., M.S., J.R., O.P., J.G.S., C.E.S.), Harvard Medical School, Boston, MA
| | - Manuel Schmid
- From the Department of Genetics (C.N.T., A.S., A.C.G., M.N., J.A.L.W., R.A., M.S., J.R., O.P., J.G.S., C.E.S.), Harvard Medical School, Boston, MA
- Deutsches Herzzentrum München, Technische Universität München, Germany (M.S.)
| | - Jyoti Rao
- From the Department of Genetics (C.N.T., A.S., A.C.G., M.N., J.A.L.W., R.A., M.S., J.R., O.P., J.G.S., C.E.S.), Harvard Medical School, Boston, MA
- Department of Pathology (J.R., O.P.), Brigham and Women’s Hospital, Boston, MA
- Harvard Stem Cell Institute, Boston, MA (J.R., O.P.)
| | - Jourdan Ewoldt
- Biomedical Engineering, Boston University, MA (J.E., A.C., C.S.C.)
- The Wyss Institute for Biologically Inspired Engineering at Harvard University, Boston, MA (J.E., A.C., C.S.C.)
| | - Olivier Pourquié
- From the Department of Genetics (C.N.T., A.S., A.C.G., M.N., J.A.L.W., R.A., M.S., J.R., O.P., J.G.S., C.E.S.), Harvard Medical School, Boston, MA
- Department of Pathology (J.R., O.P.), Brigham and Women’s Hospital, Boston, MA
- Harvard Stem Cell Institute, Boston, MA (J.R., O.P.)
| | - Anant Chopra
- Biomedical Engineering, Boston University, MA (J.E., A.C., C.S.C.)
- The Wyss Institute for Biologically Inspired Engineering at Harvard University, Boston, MA (J.E., A.C., C.S.C.)
| | - Christopher S. Chen
- Biomedical Engineering, Boston University, MA (J.E., A.C., C.S.C.)
- The Wyss Institute for Biologically Inspired Engineering at Harvard University, Boston, MA (J.E., A.C., C.S.C.)
| | - Jonathan G. Seidman
- From the Department of Genetics (C.N.T., A.S., A.C.G., M.N., J.A.L.W., R.A., M.S., J.R., O.P., J.G.S., C.E.S.), Harvard Medical School, Boston, MA
| | - Christine E. Seidman
- From the Department of Genetics (C.N.T., A.S., A.C.G., M.N., J.A.L.W., R.A., M.S., J.R., O.P., J.G.S., C.E.S.), Harvard Medical School, Boston, MA
- Cardiovascular Division, Department of Medicine (C.E.S.), Brigham and Women’s Hospital, Boston, MA
- Howard Hughes Medical Institute, Chevy Chase, MD (C.E.S.)
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17
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Matsuura R, Miyagawa S, Fukushima S, Goto T, Harada A, Shimozaki Y, Yamaki K, Sanami S, Kikuta J, Ishii M, Sawa Y. Intravital imaging with two-photon microscopy reveals cellular dynamics in the ischeamia-reperfused rat heart. Sci Rep 2018; 8:15991. [PMID: 30375442 PMCID: PMC6207786 DOI: 10.1038/s41598-018-34295-w] [Citation(s) in RCA: 25] [Impact Index Per Article: 4.2] [Reference Citation Analysis] [Abstract] [MESH Headings] [Track Full Text] [Download PDF] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Received: 01/15/2018] [Accepted: 10/09/2018] [Indexed: 12/27/2022] Open
Abstract
Recent advances in intravital microscopy have provided insight into dynamic biological events at the cellular level in both healthy and pathological tissue. However, real-time in vivo cellular imaging of the beating heart has not been fully established, mainly due to the difficulty of obtaining clear images through cycles of cardiac and respiratory motion. Here we report the successful recording of clear in vivo moving images of the beating rat heart by two-photon microscopy facilitated by cardiothoracic surgery and a novel cardiac stabiliser. Subcellular dynamics of the major cardiac components including the myocardium and its subcellular structures (i.e., nuclei and myofibrils) and mitochondrial distribution in cardiac myocytes were visualised for 4-5 h in green fluorescent protein-expressing transgenic Lewis rats at 15 frames/s. We also observed ischaemia/reperfusion (I/R) injury-induced suppression of the contraction/relaxation cycle and the consequent increase in cell permeability and leukocyte accumulation in cardiac tissue. I/R injury was induced in other transgenic mouse lines to further clarify the biological events in cardiac tissue. This imaging system can serve as an alternative modality for real time monitoring in animal models and cardiological drug screening, and can contribute to the development of more effective treatments for cardiac diseases.
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Affiliation(s)
- Ryohei Matsuura
- Department of Cardiovascular Surgery, Osaka University Graduate School of Medicine, Osaka, Japan.
| | - Shigeru Miyagawa
- Department of Cardiovascular Surgery, Osaka University Graduate School of Medicine, Osaka, Japan
| | - Satsuki Fukushima
- Department of Cardiovascular Surgery, Osaka University Graduate School of Medicine, Osaka, Japan
| | - Takasumi Goto
- Department of Cardiovascular Surgery, Osaka University Graduate School of Medicine, Osaka, Japan
| | - Akima Harada
- Department of Cardiovascular Surgery, Osaka University Graduate School of Medicine, Osaka, Japan
| | - Yuri Shimozaki
- Research and Development Division for Advanced Technology, Research and Development Center, Dai Nippon Printing Co., Ltd., Tokyo, Japan
| | - Kazumasa Yamaki
- Research and Development Division for Advanced Technology, Research and Development Center, Dai Nippon Printing Co., Ltd., Tokyo, Japan
| | - Sho Sanami
- Research and Development Division for Advanced Technology, Research and Development Center, Dai Nippon Printing Co., Ltd., Tokyo, Japan
| | - Junichi Kikuta
- Department of Immunology and Cell Biology, Osaka University Graduate School of Medicine, Osaka, Japan
| | - Masaru Ishii
- Department of Immunology and Cell Biology, Osaka University Graduate School of Medicine, Osaka, Japan
| | - Yoshiki Sawa
- Department of Cardiovascular Surgery, Osaka University Graduate School of Medicine, Osaka, Japan
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18
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Amdursky N, Mazo MM, Thomas MR, Humphrey EJ, Puetzer JL, St-Pierre JP, Skaalure SC, Richardson RM, Terracciano CM, Stevens MM. Elastic serum-albumin based hydrogels: mechanism of formation and application in cardiac tissue engineering. J Mater Chem B 2018; 6:5604-5612. [PMID: 30283632 PMCID: PMC6166857 DOI: 10.1039/c8tb01014e] [Citation(s) in RCA: 28] [Impact Index Per Article: 4.7] [Reference Citation Analysis] [Abstract] [Grants] [Track Full Text] [Download PDF] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Indexed: 12/23/2022]
Abstract
Hydrogels are promising materials for mimicking the extra-cellular environment. Here, we present a simple methodology for the formation of a free-standing viscoelastic hydrogel from the abundant and low cost protein serum albumin. We show that the mechanical properties of the hydrogel exhibit a complicated behaviour as a function of the weight fraction of the protein component. We further use X-ray scattering to shed light on the mechanism of gelation from the formation of a fibrillary network at low weight fractions to interconnected aggregates at higher weight fractions. Given the match between our hydrogel elasticity and that of the myocardium, we investigated its potential for supporting cardiac cells in vitro. Interestingly, these hydrogels support the formation of several layers of myocytes and significantly promote the maintenance of a native-like gene expression profile compared to those cultured on glass. When confronted with a multicellular ventricular cell preparation, the hydrogels can support macroscopically contracting cardiac-like tissues with a distinct cell arrangement, and form mm-long vascular-like structures. We envisage that our simple approach for the formation of an elastic substrate from an abundant protein makes the hydrogel a compelling biomedical material candidate for a wide range of cell types.
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Affiliation(s)
- Nadav Amdursky
- Department of Materials, Department of Bioengineering and Institute of Biomedical Engineering, Imperial College Lodon, London, SW7 2AZ, UK
| | - Manuel M. Mazo
- Department of Materials, Department of Bioengineering and Institute of Biomedical Engineering, Imperial College Lodon, London, SW7 2AZ, UK
| | - Michael R. Thomas
- Department of Materials, Department of Bioengineering and Institute of Biomedical Engineering, Imperial College Lodon, London, SW7 2AZ, UK
| | - Eleanor J. Humphrey
- National Heart and Lung Institute, Imperial Centre for Translational and Experimental Medicine, Imperial College London, London, SW7 2AZ, UK
| | - Jennifer L. Puetzer
- Department of Materials, Department of Bioengineering and Institute of Biomedical Engineering, Imperial College Lodon, London, SW7 2AZ, UK
| | - Jean-Philippe St-Pierre
- Department of Materials, Department of Bioengineering and Institute of Biomedical Engineering, Imperial College Lodon, London, SW7 2AZ, UK
| | - Stacey C. Skaalure
- Department of Materials, Department of Bioengineering and Institute of Biomedical Engineering, Imperial College Lodon, London, SW7 2AZ, UK
| | | | - Cesare M. Terracciano
- National Heart and Lung Institute, Imperial Centre for Translational and Experimental Medicine, Imperial College London, London, SW7 2AZ, UK
| | - Molly M. Stevens
- Department of Materials, Department of Bioengineering and Institute of Biomedical Engineering, Imperial College Lodon, London, SW7 2AZ, UK
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19
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Jackman C, Li H, Bursac N. Long-term contractile activity and thyroid hormone supplementation produce engineered rat myocardium with adult-like structure and function. Acta Biomater 2018; 78:98-110. [PMID: 30086384 DOI: 10.1016/j.actbio.2018.08.003] [Citation(s) in RCA: 31] [Impact Index Per Article: 5.2] [Reference Citation Analysis] [Abstract] [Key Words] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Received: 05/08/2018] [Revised: 08/02/2018] [Accepted: 08/03/2018] [Indexed: 02/07/2023]
Abstract
The field of cardiac tissue engineering has developed rapidly, but structural and functional immaturity of engineered heart tissues hinder their widespread use. Here, we show that a combination of low-rate (0.2 Hz) contractile activity and thyroid hormone (T3) supplementation significantly promote structural and functional maturation of engineered rat cardiac tissues ("cardiobundles"). The progressive maturation of cardiobundles during first 2 weeks of culture resulted in cell cycle exit and loss of spontaneous activity, which in longer culture yielded decreased contractile function. Maintaining a low level of contractile activity by 0.2 Hz pacing between culture weeks 3 and 5, combined with T3 treatment, yielded significant growth of cardiobundle and myocyte cross-sectional areas (by 68% and 32%, respectively), increased nuclei numbers (by 22%), improved twitch force (by 39%), shortened action potential duration (by 32%), polarized N-cadherin distribution, and switch from immature (slow skeletal) to mature (fast) cardiac troponin I isoform expression. Along with advanced functional output (conduction velocity 53.7 ± 0.8 cm/s, specific force 70.1 ± 5.8 mN/mm2), quantitative ultrastructural analyses revealed similar metrics and abundance of sarcomeres, T-tubules, M-bands, and intercalated disks compared to native age-matched (5-week) and adult (3-month) ventricular myocytes. Unlike 0.2 Hz regime, chronic 1 Hz pacing resulted in significant cardiomyocyte loss and formation of necrotic core despite the use of dynamic culture. Overall, our results demonstrate remarkable ultrastructural and functional maturation of neonatal rat cardiomyocytes in 3D culture and reveal importance of combined biophysical and hormonal inputs for in vitro engineering of adult-like myocardium. STATEMENT OF SIGNIFICANCE Compared to human stem cell-derived cardiomyocytes, neonatal rat ventricular myocytes show advanced maturation state which makes them suitable for in vitro studies of postnatal cardiac development. Still, maturation process from a neonatal to an adult cardiomyocyte has not been recapitulated in rodent cell cultures. Here, we show that low-frequency pacing and thyroid hormone supplementation of 3D engineered neonatal rat cardiac tissues synergistically yield significant increase in cell and tissue volume, robust formation of T-tubules and M-lines, improved sarcomere organization, and faster and more forceful contractions. To the best of our knowledge, 5-week old engineered cardiac tissues described in this study are the first that exhibit both ultrastructural and functional characteristics approaching or matching those of adult ventricular myocardium.
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20
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Optimization of Fluorescent Labeling for In Vivo Nanoimaging of Sarcomeres in the Mouse Heart. BIOMED RESEARCH INTERNATIONAL 2018; 2018:4349170. [PMID: 30211223 PMCID: PMC6126089 DOI: 10.1155/2018/4349170] [Citation(s) in RCA: 4] [Impact Index Per Article: 0.7] [Reference Citation Analysis] [Abstract] [Track Full Text] [Download PDF] [Figures] [Subscribe] [Scholar Register] [Received: 03/27/2018] [Accepted: 06/13/2018] [Indexed: 11/18/2022]
Abstract
The present study was conducted to systematically investigate the optimal viral titer as well as the volume of the adenovirus vector (ADV) that expresses α-actinin-AcGFP in the Z-disks of myocytes in the left ventricle (LV) of mice. An injection of 10 μL ADV at viral titers of 2 to 4 × 1011 viral particles per mL (VP/mL) into the LV epicardial surface consistently expressed α-actinin-AcGFP in myocytes in vivo, with the fraction of AcGFP-expressing myocytes at ~10%. Our analysis revealed that SL was ~1.90-2.15 μm upon heart arrest via deep anesthesia. Likewise, we developed a novel fluorescence labeling method of the T-tubular system by treating the LV surface with CellMask Orange (CellMask). We found that the T-tubular distance was ~2.10-2.25 μm, similar to SL, in the healthy heart in vivo. Therefore, the present high-precision visualization method for the Z-disks or the T-tubules is beneficial to unveiling the mechanisms of myocyte contraction in health and disease in vivo.
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21
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Chatterjee K, Pratiwi FW, Wu FCM, Chen P, Chen BC. Recent Progress in Light Sheet Microscopy for Biological Applications. APPLIED SPECTROSCOPY 2018; 72:1137-1169. [PMID: 29926744 DOI: 10.1177/0003702818778851] [Citation(s) in RCA: 28] [Impact Index Per Article: 4.7] [Reference Citation Analysis] [Abstract] [Key Words] [MESH Headings] [Track Full Text] [Subscribe] [Scholar Register] [Indexed: 06/08/2023]
Abstract
The introduction of light sheet fluorescence microscopy (LSFM) has overcome the challenges in conventional optical microscopy. Among the recent breakthroughs in fluorescence microscopy, LSFM had been proven to provide a high three-dimensional spatial resolution, high signal-to-noise ratio, fast imaging acquisition rate, and minuscule levels of phototoxic and photodamage effects. The aforementioned auspicious properties are crucial in the biomedical and clinical research fields, covering a broad range of applications: from the super-resolution imaging of intracellular dynamics in a single cell to the high spatiotemporal resolution imaging of developmental dynamics in an entirely large organism. In this review, we provided a systematic outline of the historical development of LSFM, detailed discussion on the variants and improvements of LSFM, and delineation on the most recent technological advancements of LSFM and its potential applications in single molecule/particle detection, single-molecule super-resolution imaging, imaging intracellular dynamics of a single cell, multicellular imaging: cell-cell and cell-matrix interactions, plant developmental biology, and brain imaging and developmental biology.
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Affiliation(s)
- Krishnendu Chatterjee
- 1 Nanoscience and Technology Program, Taiwan International Graduate Program, Academia Sinica, Taipei, Taiwan
- 2 Research Center for Applied Sciences, Academia Sinica, Taipei, Taiwan
- 3 Department of Engineering and System Science, National Tsing-Hua University, Hsinchu, Taiwan
| | - Feby Wijaya Pratiwi
- 1 Nanoscience and Technology Program, Taiwan International Graduate Program, Academia Sinica, Taipei, Taiwan
- 2 Research Center for Applied Sciences, Academia Sinica, Taipei, Taiwan
- 4 Department of Chemistry, National Taiwan University, Taipei, Taiwan
| | | | - Peilin Chen
- 2 Research Center for Applied Sciences, Academia Sinica, Taipei, Taiwan
| | - Bi-Chang Chen
- 2 Research Center for Applied Sciences, Academia Sinica, Taipei, Taiwan
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22
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Limpitikul WB, Viswanathan MC, O'Rourke B, Yue DT, Cammarato A. Conservation of cardiac L-type Ca 2+ channels and their regulation in Drosophila: A novel genetically-pliable channelopathic model. J Mol Cell Cardiol 2018; 119:64-74. [PMID: 29684406 PMCID: PMC6154789 DOI: 10.1016/j.yjmcc.2018.04.010] [Citation(s) in RCA: 5] [Impact Index Per Article: 0.8] [Reference Citation Analysis] [Abstract] [MESH Headings] [Grants] [Track Full Text] [Journal Information] [Submit a Manuscript] [Subscribe] [Scholar Register] [Received: 11/10/2017] [Revised: 04/08/2018] [Accepted: 04/11/2018] [Indexed: 01/28/2023]
Abstract
Dysregulation of L-type Ca2+ channels (LTCCs) underlies numerous cardiac pathologies. Understanding their modulation with high fidelity relies on investigating LTCCs in their native environment with intact interacting proteins. Such studies benefit from genetic manipulation of endogenous channels in cardiomyocytes, which often proves cumbersome in mammalian models. Drosophila melanogaster, however, offers a potentially efficient alternative as it possesses a relatively simple heart, is genetically pliable, and expresses well-conserved genes. Fluorescence in situ hybridization confirmed an abundance of Ca-α1D and Ca-α1T mRNA in fly myocardium, which encode subunits that specify hetero-oligomeric channels homologous to mammalian LTCCs and T-type Ca2+ channels, respectively. Cardiac-specific knockdown of Ca-α1D via interfering RNA abolished cardiac contraction, suggesting Ca-α1D (i.e. A1D) represents the primary functioning Ca2+ channel in Drosophila hearts. Moreover, we successfully isolated viable single cardiomyocytes and recorded Ca2+ currents via patch clamping, a feat never before accomplished with the fly model. The profile of Ca2+ currents recorded in individual cells when Ca2+ channels were hypomorphic, absent, or under selective LTCC blockage by nifedipine, additionally confirmed the predominance of A1D current across all activation voltages. T-type current, activated at more negative voltages, was also detected. Lastly, A1D channels displayed Ca2+-dependent inactivation, a critical negative feedback mechanism of LTCCs, and the current through them was augmented by forskolin, an activator of the protein kinase A pathway. In sum, the Drosophila heart possesses a conserved compendium of Ca2+ channels, suggesting that the fly may serve as a robust and effective platform for studying cardiac channelopathies.
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Affiliation(s)
- Worawan B Limpitikul
- Calcium Signals Laboratory, Department of Biomedical Engineering, The Johns Hopkins University School of Medicine, Ross Research Building, 720 Rutland Avenue, Baltimore, MD 21205, United States
| | - Meera C Viswanathan
- Institute of CardioScience, Division of Cardiology, Department of Medicine, The Johns Hopkins University School of Medicine, Ross Research Building, 720 Rutland Avenue, Baltimore, MD 21205, United States
| | - Brian O'Rourke
- Institute of CardioScience, Division of Cardiology, Department of Medicine, The Johns Hopkins University School of Medicine, Ross Research Building, 720 Rutland Avenue, Baltimore, MD 21205, United States
| | - David T Yue
- Calcium Signals Laboratory, Department of Biomedical Engineering, The Johns Hopkins University School of Medicine, Ross Research Building, 720 Rutland Avenue, Baltimore, MD 21205, United States
| | - Anthony Cammarato
- Institute of CardioScience, Division of Cardiology, Department of Medicine, The Johns Hopkins University School of Medicine, Ross Research Building, 720 Rutland Avenue, Baltimore, MD 21205, United States; Department of Physiology, The Johns Hopkins University School of Medicine, Ross Research Building, 720 Rutland Avenue, Baltimore, MD 21205, United States.
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23
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Burton RAB, Rog-Zielinska EA, Corbett AD, Peyronnet R, Bodi I, Fink M, Sheldon J, Hoenger A, Calaghan SC, Bub G, Kohl P. Caveolae in Rabbit Ventricular Myocytes: Distribution and Dynamic Diminution after Cell Isolation. Biophys J 2017; 113:1047-1059. [PMID: 28877488 PMCID: PMC5653872 DOI: 10.1016/j.bpj.2017.07.026] [Citation(s) in RCA: 21] [Impact Index Per Article: 3.0] [Reference Citation Analysis] [Abstract] [Track Full Text] [Download PDF] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Received: 02/28/2016] [Revised: 05/16/2017] [Accepted: 07/06/2017] [Indexed: 12/12/2022] Open
Abstract
Caveolae are signal transduction centers, yet their subcellular distribution and preservation in cardiac myocytes after cell isolation are not well documented. Here, we quantify caveolae located within 100 nm of the outer cell surface membrane in rabbit single-ventricular cardiomyocytes over 8 h post-isolation and relate this to the presence of caveolae in intact tissue. Hearts from New Zealand white rabbits were either chemically fixed by coronary perfusion or enzymatically digested to isolate ventricular myocytes, which were subsequently fixed at 0, 3, and 8 h post-isolation. In live cells, the patch-clamp technique was used to measure whole-cell plasma membrane capacitance, and in fixed cells, caveolae were quantified by transmission electron microscopy. Changes in cell-surface topology were assessed using scanning electron microscopy. In fixed ventricular myocardium, dual-axis electron tomography was used for three-dimensional reconstruction and analysis of caveolae in situ. The presence and distribution of surface-sarcolemmal caveolae in freshly isolated cells matches that of intact myocardium. With time, the number of surface-sarcolemmal caveolae decreases in isolated cardiomyocytes. This is associated with a gradual increase in whole-cell membrane capacitance. Concurrently, there is a significant increase in area, diameter, and circularity of sub-sarcolemmal mitochondria, indicative of swelling. In addition, electron tomography data from intact heart illustrate the regular presence of caveolae not only at the surface sarcolemma, but also on transverse-tubular membranes in ventricular myocardium. Thus, caveolae are dynamic structures, present both at surface-sarcolemmal and transverse-tubular membranes. After cell isolation, the number of surface-sarcolemmal caveolae decreases significantly within a time frame relevant for single-cell research. The concurrent increase in cell capacitance suggests that membrane incorporation of surface-sarcolemmal caveolae underlies this, but internalization and/or micro-vesicle loss to the extracellular space may also contribute. Given that much of the research into cardiac caveolae-dependent signaling utilizes isolated cells, and since caveolae-dependent pathways matter for a wide range of other study targets, analysis of isolated cell data should take the time post-isolation into account.
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Affiliation(s)
- Rebecca A B Burton
- Department of Pharmacology, University of Oxford, Oxford, United Kingdom
| | - Eva A Rog-Zielinska
- National Heart and Lung Institute, Imperial College London, London, United Kingdom; Institute for Experimental Cardiovascular Medicine, University Heart Center Freiburg-Bad Krozingen, Faculty of Medicine, University of Freiburg, Freiburg, Germany.
| | | | - Rémi Peyronnet
- Institute for Experimental Cardiovascular Medicine, University Heart Center Freiburg-Bad Krozingen, Faculty of Medicine, University of Freiburg, Freiburg, Germany
| | - Ilona Bodi
- Institute for Experimental Cardiovascular Medicine, University Heart Center Freiburg-Bad Krozingen, Faculty of Medicine, University of Freiburg, Freiburg, Germany
| | - Martin Fink
- Department of Physiology, Anatomy and Genetics, University of Oxford, Oxford, United Kingdom
| | - Judith Sheldon
- Department of Physiology, Anatomy and Genetics, University of Oxford, Oxford, United Kingdom
| | - Andreas Hoenger
- Department of Molecular, Cellular and Developmental Biology, University of Colorado, Boulder, Colorado
| | - Sarah C Calaghan
- School of Biomedical Sciences, University of Leeds, Leeds, United Kingdom
| | - Gil Bub
- Department of Physiology, Anatomy and Genetics, University of Oxford, Oxford, United Kingdom
| | - Peter Kohl
- Institute for Experimental Cardiovascular Medicine, University Heart Center Freiburg-Bad Krozingen, Faculty of Medicine, University of Freiburg, Freiburg, Germany
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24
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Peyronnet R, Bollensdorff C, Capel RA, Rog-Zielinska EA, Woods CE, Charo DN, Lookin O, Fajardo G, Ho M, Quertermous T, Ashley EA, Kohl P. Load-dependent effects of apelin on murine cardiomyocytes. PROGRESS IN BIOPHYSICS AND MOLECULAR BIOLOGY 2017; 130:333-343. [PMID: 28935153 PMCID: PMC5726609 DOI: 10.1016/j.pbiomolbio.2017.09.013] [Citation(s) in RCA: 17] [Impact Index Per Article: 2.4] [Reference Citation Analysis] [Abstract] [Key Words] [Track Full Text] [Download PDF] [Figures] [Subscribe] [Scholar Register] [Received: 08/13/2017] [Revised: 09/07/2017] [Accepted: 09/08/2017] [Indexed: 01/26/2023]
Abstract
The apelin peptide is described as one of the most potent inotropic agents, produced endogenously in a wide range of cells, including cardiomyocytes. Despite positive effects on cardiac contractility in multicellular preparations, as well as indications of cardio-protective actions in several diseases, its effects and mechanisms of action at the cellular level are incompletely understood. Here, we report apelin effects on dynamic mechanical characteristics of single ventricular cardiomyocytes, isolated from mouse models (control, apelin-deficient [Apelin-KO], apelin-receptor KO mouse [APJ-KO]), and rat. Dynamic changes in maximal velocity of cell shortening and relaxation were monitored. In addition, more traditional indicators of inotropic effects, such as maximum shortening (in mechanically unloaded cells) or peak force development (in auxotonic contracting cells, preloaded using the carbon fibre technique) were studied. The key finding is that, using Apelin-KO cardiomyocytes exposed to different preloads with the 2-carbon fibre technique, we observe a lowering of the slope of the end-diastolic stress-length relation in response to 10 nM apelin, an effect that is preload-dependent. This suggests a positive lusitropic effect of apelin, which could explain earlier counter-intuitive findings on an apelin-induced increase in contractility occurring without matching rise in oxygen consumption.
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Affiliation(s)
- Rémi Peyronnet
- Institute for Experimental Cardiovascular Medicine, University Heart Centre Freiburg · Bad Krozingen, Medical School of the University of Freiburg, Germany; Imperial College London, NHLI, Heart Science Centre, UK.
| | - Christian Bollensdorff
- Imperial College London, NHLI, Heart Science Centre, UK; Sidra Medical and Research Center, Qatar Foundation, Qatar
| | | | - Eva A Rog-Zielinska
- Institute for Experimental Cardiovascular Medicine, University Heart Centre Freiburg · Bad Krozingen, Medical School of the University of Freiburg, Germany; Imperial College London, NHLI, Heart Science Centre, UK
| | - Christopher E Woods
- Stanford University Division of Cardiovascular Medicine, Stanford, USA; Palo Alto Medical Foundation, Burlingame, CA, USA
| | - David N Charo
- Stanford University Division of Cardiovascular Medicine, Stanford, USA
| | - Oleg Lookin
- Ural Branch of the Russian Academy of Sciences, Ekaterinburg, Russian Federation
| | - Giovanni Fajardo
- Stanford University Division of Cardiovascular Medicine, Stanford, USA
| | - Michael Ho
- Stanford University Division of Cardiovascular Medicine, Stanford, USA
| | | | - Euan A Ashley
- Stanford University Division of Cardiovascular Medicine, Stanford, USA
| | - Peter Kohl
- Institute for Experimental Cardiovascular Medicine, University Heart Centre Freiburg · Bad Krozingen, Medical School of the University of Freiburg, Germany; Imperial College London, NHLI, Heart Science Centre, UK
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25
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Hansen KJ, Favreau JT, Gershlak JR, Laflamme MA, Albrecht DR, Gaudette GR. Optical Method to Quantify Mechanical Contraction and Calcium Transients of Human Pluripotent Stem Cell-Derived Cardiomyocytes. Tissue Eng Part C Methods 2017; 23:445-454. [PMID: 28562232 DOI: 10.1089/ten.tec.2017.0190] [Citation(s) in RCA: 14] [Impact Index Per Article: 2.0] [Reference Citation Analysis] [Abstract] [Key Words] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Indexed: 01/14/2023] Open
Abstract
Differentiation of human pluripotent stem cells into cardiomyocytes (hPS-CMs) holds promise for myocardial regeneration therapies, drug discovery, and models of cardiac disease. Potential cardiotoxicities may affect hPS-CM mechanical contraction independent of calcium signaling. Herein, a method using an image capture system is described to measure hPS-CM contractility and intracellular calcium concurrently, with high spatial and temporal resolution. The image capture system rapidly alternates between brightfield and epifluorescent illumination of contracting cells. Mechanical contraction is quantified by a speckle tracking algorithm applied to brightfield image pairs, whereas calcium transients are measured by a fluorescent calcium reporter. This technique captured changes in contractile strain, calcium transients, and beat frequency of hPS-CMs over 21 days in culture, as well as acute responses to isoproterenol and Cytochalasin D. The technique described above can be applied without the need to alter the culture platform, allowing for determination of hPS-CM behavior over weeks in culture for drug discovery and myocardial regeneration applications.
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Affiliation(s)
- Katrina J Hansen
- 1 Department of Biomedical Engineering, Worcester Polytechnic Institute , Worcester, Massachusetts
| | - John T Favreau
- 1 Department of Biomedical Engineering, Worcester Polytechnic Institute , Worcester, Massachusetts
| | - Joshua R Gershlak
- 1 Department of Biomedical Engineering, Worcester Polytechnic Institute , Worcester, Massachusetts
| | - Michael A Laflamme
- 2 Toronto General Research Institute, McEwen Centre for Regenerative Medicine, University Health Network , Toronto, Canada
| | - Dirk R Albrecht
- 1 Department of Biomedical Engineering, Worcester Polytechnic Institute , Worcester, Massachusetts
| | - Glenn R Gaudette
- 1 Department of Biomedical Engineering, Worcester Polytechnic Institute , Worcester, Massachusetts
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26
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Abdelsalam DG, Yasui T. High brightness, low coherence, digital holographic microscopy for 3D visualization of an in-vitro sandwiched biological sample. APPLIED OPTICS 2017; 56:F1-F6. [PMID: 28463291 DOI: 10.1364/ao.56.0000f1] [Citation(s) in RCA: 0] [Impact Index Per Article: 0] [Reference Citation Analysis] [Abstract] [MESH Headings] [Track Full Text] [Subscribe] [Scholar Register] [Received: 10/28/2016] [Accepted: 12/20/2016] [Indexed: 06/07/2023]
Abstract
We achieve practically a bright-field digital holographic microscopy (DHM) configuration free from coherent noise for three-dimensional (3D) visualization of an in-vitro sandwiched sarcomere sample. Visualization of such sandwiched samples by conventional atomic force microscope (AFM) is impossible, while visualization using DHM with long coherent lengths is challenging. The proposed configuration is comprised of an ultrashort pulse laser source and a Mach-Zehnder interferometer in transmission. Periodically poled lithium niobate (PPLN) crystal was used to convert the fundamental beam by second harmonic generation (SHG) to the generated beam fit to the CCD camera used. The experimental results show that the contrast of the reconstructed phase image is improved to a higher degree compared to a He-Ne laser based result. We attribute this improvement to two things: the feature of the femtosecond pulse light, which acts as a chopper for coherent noise suppression, and the fact that the variance of a coherent mode can be reduced by a factor of 9 due to low loss through a nonlinear medium.
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27
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Casero R, Siedlecka U, Jones ES, Gruscheski L, Gibb M, Schneider JE, Kohl P, Grau V. Transformation diffusion reconstruction of three-dimensional histology volumes from two-dimensional image stacks. Med Image Anal 2017; 38:184-204. [PMID: 28411458 PMCID: PMC5408912 DOI: 10.1016/j.media.2017.03.004] [Citation(s) in RCA: 13] [Impact Index Per Article: 1.9] [Reference Citation Analysis] [Abstract] [Key Words] [Track Full Text] [Download PDF] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Received: 07/13/2016] [Revised: 03/15/2017] [Accepted: 03/21/2017] [Indexed: 12/05/2022]
Abstract
A method for 3D reconstruction of serial 2D histology image stacks is proposed. Pre-alignment to an external pre-cut reference (blockface) prevents shape artifacts. Formulated as diffusion of transformations from each slice to its neighbors. Registrations replaced by much faster transformation operations.
Traditional histology is the gold standard for tissue studies, but it is intrinsically reliant on two-dimensional (2D) images. Study of volumetric tissue samples such as whole hearts produces a stack of misaligned and distorted 2D images that need to be reconstructed to recover a congruent volume with the original sample's shape. In this paper, we develop a mathematical framework called Transformation Diffusion (TD) for stack alignment refinement as a solution to the heat diffusion equation. This general framework does not require contour segmentation, is independent of the registration method used, and is trivially parallelizable. After the first stack sweep, we also replace registration operations by operations in the space of transformations, several orders of magnitude faster and less memory-consuming. Implementing TD with operations in the space of transformations produces our Transformation Diffusion Reconstruction (TDR) algorithm, applicable to general transformations that are closed under inversion and composition. In particular, we provide formulas for translation and affine transformations. We also propose an Approximated TDR (ATDR) algorithm that extends the same principles to tensor-product B-spline transformations. Using TDR and ATDR, we reconstruct a full mouse heart at pixel size 0.92 µm × 0.92 µm, cut 10 µm thick, spaced 20 µm (84G). Our algorithms employ only local information from transformations between neighboring slices, but the TD framework allows theoretical analysis of the refinement as applying a global Gaussian low-pass filter to the unknown stack misalignments. We also show that reconstruction without an external reference produces large shape artifacts in a cardiac specimen while still optimizing slice-to-slice alignment. To overcome this problem, we use a pre-cutting blockface imaging process previously developed by our group that takes advantage of Brewster's angle and a polarizer to capture the outline of only the topmost layer of wax in the block containing embedded tissue for histological sectioning.
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Affiliation(s)
- Ramón Casero
- Institute of Biomedical Engineering, Department of Engineering Science, University of Oxford, Oxford OX3 7DQ, UK.
| | - Urszula Siedlecka
- Heart Science Centre, National Lung and Heart Institute, Imperial College London, Harefield UB9 6JH, UK
| | - Elizabeth S Jones
- Heart Science Centre, National Lung and Heart Institute, Imperial College London, Harefield UB9 6JH, UK
| | - Lena Gruscheski
- Heart Science Centre, National Lung and Heart Institute, Imperial College London, Harefield UB9 6JH, UK
| | - Matthew Gibb
- Institute of Biomedical Engineering, Department of Engineering Science, University of Oxford, Oxford OX3 7DQ, UK
| | - Jürgen E Schneider
- BHF Experimental MR Unit, Division of Cardiovascular Medicine, Wellcome Trust Centre for Human Genetics, University of Oxford, Oxford OX3 7BN, UK
| | - Peter Kohl
- Institute for Experimental Cardiovascular Medicine, University Heart Centre Freiburg - Bad Krozingen, School of Medicine, University of Freiburg, Elsässer Str 2Q, 79110 Freiburg, Germany
| | - Vicente Grau
- Institute of Biomedical Engineering, Department of Engineering Science, University of Oxford, Oxford OX3 7DQ, UK
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28
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Huethorst E, Hortigon M, Zamora-Rodriguez V, Reynolds PM, Burton F, Smith G, Gadegaard N. Enhanced Human-Induced Pluripotent Stem Cell Derived Cardiomyocyte Maturation Using a Dual Microgradient Substrate. ACS Biomater Sci Eng 2016; 2:2231-2239. [PMID: 27990488 PMCID: PMC5155309 DOI: 10.1021/acsbiomaterials.6b00426] [Citation(s) in RCA: 27] [Impact Index Per Article: 3.4] [Reference Citation Analysis] [Abstract] [Key Words] [Track Full Text] [Download PDF] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Received: 07/26/2016] [Accepted: 10/17/2016] [Indexed: 12/29/2022]
Abstract
Human-induced pluripotent stem cell-derived cardiomyocytes (hiPSC-CM) raise many possibilities for cardiac research but they exhibit an immature phenotype, which influences experimental outcomes. The aim of our research is to investigate the effects of a topographical gradient substrate on the morphology and function of commercially available hiPSC-CM. The lateral dimensions the microgrooves on the substrate varied from 8 to 100 μm space between the 8 μm grooves on one axis and from ∼5 nm to ∼1 μm in depth on the other axis. Cells were seeded homogeneously across the substrate and according to the manufacturers protocols. At days 4 and 10, measures of eccentricity, elongation, orientation, sarcomere length (SL), and contractility of the hiPSC-CM were taken. Only the deepest and widest region (8-30 μm wide and 0.85-1 μm deep) showed a significantly higher percentage of hiPSC-CM with an increased eccentricity (31.3 ± 6.4%), elongation (10.4 ± 4.3%), and orientation (<10°) (32.1 ± 2.7%) when compared with the control (flat substrate) (15.8 ± 5.0%, 3.4 ± 2.7%, and 10.6 ± 1.1%, respectively). Additionally, during stimulus-induced contraction, the relaxation phase of the twitch was prolonged (400 ms) compared to nonelongated cells (200 ms). These findings support the potential use of dual microgradient substrates to investigate substrate topographies that stimulate migration and/or maturation of hiPSC-CM.
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Affiliation(s)
- E Huethorst
- Institute of Cardiovascular and Medical Sciences, University of Glasgow, Glasgow G12 8QQ, United Kingdom; Division of Biomedical Engineering, School of Engineering, University of Glasgow, Glasgow G12 8LT, United Kingdom
| | - M Hortigon
- Institute of Cardiovascular and Medical Sciences, University of Glasgow , Glasgow G12 8QQ, United Kingdom
| | - V Zamora-Rodriguez
- Institute of Cardiovascular and Medical Sciences, University of Glasgow , Glasgow G12 8QQ, United Kingdom
| | - P M Reynolds
- Division of Biomedical Engineering, School of Engineering, University of Glasgow , Glasgow G12 8LT, United Kingdom
| | - F Burton
- Institute of Cardiovascular and Medical Sciences, University of Glasgow , Glasgow G12 8QQ, United Kingdom
| | - G Smith
- Institute of Cardiovascular and Medical Sciences, University of Glasgow , Glasgow G12 8QQ, United Kingdom
| | - N Gadegaard
- Division of Biomedical Engineering, School of Engineering, University of Glasgow , Glasgow G12 8LT, United Kingdom
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29
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Kobirumaki-Shimozawa F, Oyama K, Shimozawa T, Mizuno A, Ohki T, Terui T, Minamisawa S, Ishiwata S, Fukuda N. Nano-imaging of the beating mouse heart in vivo: Importance of sarcomere dynamics, as opposed to sarcomere length per se, in the regulation of cardiac function. ACTA ACUST UNITED AC 2016; 147:53-62. [PMID: 26712849 PMCID: PMC4692490 DOI: 10.1085/jgp.201511484] [Citation(s) in RCA: 42] [Impact Index Per Article: 5.3] [Reference Citation Analysis] [Abstract] [Track Full Text] [Download PDF] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Indexed: 01/25/2023]
Abstract
¡Vive la différence! In cardiac contraction, the reduction in sarcomere length—rather than length itself—determines contractile force. Sarcomeric contraction in cardiomyocytes serves as the basis for the heart’s pump functions in mammals. Although it plays a critical role in the circulatory system, myocardial sarcomere length (SL) change has not been directly measured in vivo under physiological conditions because of technical difficulties. In this study, we developed a high speed (100–frames per second), high resolution (20-nm) imaging system for myocardial sarcomeres in living mice. Using this system, we conducted three-dimensional analysis of sarcomere dynamics in left ventricular myocytes during the cardiac cycle, simultaneously with electrocardiogram and left ventricular pressure measurements. We found that (a) the working range of SL was on the shorter end of the resting distribution, and (b) the left ventricular–developed pressure was positively correlated with the SL change between diastole and systole. The present findings provide the first direct evidence for the tight coupling of sarcomere dynamics and ventricular pump functions in the physiology of the heart.
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Affiliation(s)
- Fuyu Kobirumaki-Shimozawa
- Department of Cell Physiology and Department of Anesthesiology, The Jikei University School of Medicine, Minato-ku, Tokyo 105-8461, Japan
| | - Kotaro Oyama
- Department of Cell Physiology and Department of Anesthesiology, The Jikei University School of Medicine, Minato-ku, Tokyo 105-8461, Japan Department of Physics and Department of Life Science and Medical Bioscience, School of Advanced Science and Engineering, Waseda University, Shinjuku-ku, Tokyo 169-8555, Japan
| | - Togo Shimozawa
- Department of Physics and Department of Life Science and Medical Bioscience, School of Advanced Science and Engineering, Waseda University, Shinjuku-ku, Tokyo 169-8555, Japan
| | - Akari Mizuno
- Department of Physics and Department of Life Science and Medical Bioscience, School of Advanced Science and Engineering, Waseda University, Shinjuku-ku, Tokyo 169-8555, Japan
| | - Takashi Ohki
- Department of Physics and Department of Life Science and Medical Bioscience, School of Advanced Science and Engineering, Waseda University, Shinjuku-ku, Tokyo 169-8555, Japan
| | - Takako Terui
- Department of Cell Physiology and Department of Anesthesiology, The Jikei University School of Medicine, Minato-ku, Tokyo 105-8461, Japan
| | - Susumu Minamisawa
- Department of Cell Physiology and Department of Anesthesiology, The Jikei University School of Medicine, Minato-ku, Tokyo 105-8461, Japan
| | - Shin'ichi Ishiwata
- Department of Physics and Department of Life Science and Medical Bioscience, School of Advanced Science and Engineering, Waseda University, Shinjuku-ku, Tokyo 169-8555, Japan Waseda Bioscience Research Institute in Singapore, Waseda University, Helios, Singapore 138667
| | - Norio Fukuda
- Department of Cell Physiology and Department of Anesthesiology, The Jikei University School of Medicine, Minato-ku, Tokyo 105-8461, Japan
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30
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Shimozawa T, Hirokawa E, Kobirumaki-Shimozawa F, Oyama K, Shintani SA, Terui T, Kushida Y, Tsukamoto S, Fujii T, Ishiwata S, Fukuda N. In vivo cardiac nano-imaging: A new technology for high-precision analyses of sarcomere dynamics in the heart. PROGRESS IN BIOPHYSICS AND MOLECULAR BIOLOGY 2016; 124:31-40. [PMID: 27664770 DOI: 10.1016/j.pbiomolbio.2016.09.006] [Citation(s) in RCA: 9] [Impact Index Per Article: 1.1] [Reference Citation Analysis] [Abstract] [Key Words] [Track Full Text] [Subscribe] [Scholar Register] [Received: 06/24/2016] [Revised: 09/15/2016] [Accepted: 09/20/2016] [Indexed: 12/01/2022]
Abstract
The cardiac pump function is a result of a rise in intracellular Ca2+ and the ensuing sarcomeric contractions [i.e., excitation-contraction (EC) coupling] in myocytes in various locations of the heart. In order to elucidate the heart's mechanical properties under various settings, cardiac imaging is widely performed in today's clinical as well as experimental cardiology by using echocardiogram, magnetic resonance imaging and computed tomography. However, because these common techniques detect local myocardial movements at a spatial resolution of ∼100 μm, our knowledge on the sub-cellular mechanisms of the physiology and pathophysiology of the heart in vivo is limited. This is because (1) EC coupling occurs in the μm partition in a myocyte and (2) cardiac sarcomeres generate active force upon a length change of ∼100 nm on a beat-to-beat basis. Recent advances in optical technologies have enabled measurements of intracellular Ca2+ dynamics and sarcomere length displacements at high spatial and temporal resolution in the beating heart of living rodents. Future studies with these technologies are warranted to open a new era in cardiac research.
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Affiliation(s)
- Togo Shimozawa
- Department of Life Science and Medical Bioscience, School of Advanced Science and Engineering, Waseda University, 2-2 Wakamatsu-cho, Sinjuku-ku, Tokyo 162-8480, Japan
| | - Erisa Hirokawa
- Department of Cell Physiology, The Jikei University School of Medicine, 3-25-8 Nishi-shinbashi, Minato-ku, Tokyo 105-8461, Japan
| | - Fuyu Kobirumaki-Shimozawa
- Department of Cell Physiology, The Jikei University School of Medicine, 3-25-8 Nishi-shinbashi, Minato-ku, Tokyo 105-8461, Japan
| | - Kotaro Oyama
- Department of Cell Physiology, The Jikei University School of Medicine, 3-25-8 Nishi-shinbashi, Minato-ku, Tokyo 105-8461, Japan
| | - Seine A Shintani
- Department of Physics, Graduate School of Science, The University of Tokyo, 7-3-1 Hongo Bunkyo-ku, Tokyo 113-0033, Japan
| | - Takako Terui
- Department of Anesthesiology, The Jikei University School of Medicine, 3-25-8 Nishi-shinbashi, Minato-ku, Tokyo 105-8461, Japan
| | - Yasuharu Kushida
- Department of Cell Physiology, The Jikei University School of Medicine, 3-25-8 Nishi-shinbashi, Minato-ku, Tokyo 105-8461, Japan
| | - Seiichi Tsukamoto
- Department of Cell Physiology, The Jikei University School of Medicine, 3-25-8 Nishi-shinbashi, Minato-ku, Tokyo 105-8461, Japan
| | - Teruyuki Fujii
- Department of Cell Physiology, The Jikei University School of Medicine, 3-25-8 Nishi-shinbashi, Minato-ku, Tokyo 105-8461, Japan
| | - Shin'ichi Ishiwata
- Department of Physics, Faculty of Advanced Science and Engineering, Waseda University, 3-4-1 Okubo, Shinjuku-ku, Tokyo 169-8555, Japan
| | - Norio Fukuda
- Department of Cell Physiology, The Jikei University School of Medicine, 3-25-8 Nishi-shinbashi, Minato-ku, Tokyo 105-8461, Japan.
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Woods C, Shang C, Taghavi F, Downey P, Zalewski A, Rubio GR, Liu J, Homburger JR, Grunwald Z, Qi W, Bollensdorff C, Thanaporn P, Ali A, Riemer K, Kohl P, Mochly-Rosen D, Gerstenfeld E, Large S, Ali Z, Ashley E. In Vivo Post-Cardiac Arrest Myocardial Dysfunction Is Supported by Ca2+/Calmodulin-Dependent Protein Kinase II-Mediated Calcium Long-Term Potentiation and Mitigated by Alda-1, an Agonist of Aldehyde Dehydrogenase Type 2. Circulation 2016; 134:961-977. [PMID: 27582424 DOI: 10.1161/circulationaha.116.021618] [Citation(s) in RCA: 15] [Impact Index Per Article: 1.9] [Reference Citation Analysis] [Abstract] [Key Words] [Track Full Text] [Journal Information] [Submit a Manuscript] [Subscribe] [Scholar Register] [Received: 09/10/2013] [Accepted: 07/21/2016] [Indexed: 11/16/2022]
Abstract
BACKGROUND Survival after sudden cardiac arrest is limited by postarrest myocardial dysfunction, but understanding of this phenomenon is constrained by a lack of data from a physiological model of disease. In this study, we established an in vivo model of cardiac arrest and resuscitation, characterized the biology of the associated myocardial dysfunction, and tested novel therapeutic strategies. METHODS We developed rodent models of in vivo postarrest myocardial dysfunction using extracorporeal membrane oxygenation resuscitation followed by invasive hemodynamics measurement. In postarrest isolated cardiomyocytes, we assessed mechanical load and Ca(2) (+)-induced Ca(2+) release (CICR) simultaneously using the microcarbon fiber technique and observed reduced function and myofilament calcium sensitivity. We used a novel fiberoptic catheter imaging system and a genetically encoded calcium sensor, GCaMP6f, to image CICR in vivo. RESULTS We found potentiation of CICR in isolated cells from this extracorporeal membrane oxygenation model and in cells isolated from an ischemia/reperfusion Langendorff model perfused with oxygenated blood from an arrested animal but not when reperfused in saline. We established that CICR potentiation begins in vivo. The augmented CICR observed after arrest was mediated by the activation of Ca(2+)/calmodulin-dependent protein kinase II (CaMKII). Increased phosphorylation of CaMKII, phospholamban, and ryanodine receptor 2 was detected in the postarrest period. Exogenous adrenergic activation in vivo recapitulated Ca(2+) potentiation but was associated with lesser CaMKII activation. Because oxidative stress and aldehydic adduct formation were high after arrest, we tested a small-molecule activator of aldehyde dehydrogenase type 2, Alda-1, which reduced oxidative stress, restored calcium and CaMKII homeostasis, and improved cardiac function and postarrest outcome in vivo. CONCLUSIONS Cardiac arrest and reperfusion lead to CaMKII activation and calcium long-term potentiation, which support cardiomyocyte contractility in the face of impaired postarrest myofilament calcium sensitivity. Alda-1 mitigates these effects, normalizes calcium cycling, and improves outcome.
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Affiliation(s)
- Christopher Woods
- Division of Cardiology, Arrhythmia Section, Palo Alto Medical Foundation, Burlingame, CA
| | - Ching Shang
- Division of Cardiovascular Medicine, Stanford University, Stanford, CA
| | - Fouad Taghavi
- Department of Cardiothoracic Surgery, Papworth Hospital, Cambridge, UK
| | - Peter Downey
- Division of Cardiology, Columbia University, New York, NY
| | | | - Gabriel R Rubio
- Division of Cardiovascular Medicine, Stanford University, Stanford, CA
| | - Jing Liu
- Division of Cardiovascular Medicine, Stanford University, Stanford, CA
| | | | - Zachary Grunwald
- Division of Cardiovascular Medicine, Stanford University, Stanford, CA
| | - Wei Qi
- Division of Cardiology, Columbia University, New York, NY
| | | | - Porama Thanaporn
- Division of Cardiovascular Medicine, Stanford University, Stanford, CA
| | - Ayyaz Ali
- Department of Cardiothoracic Surgery, Papworth Hospital, Cambridge, UK
| | - Kirk Riemer
- Department of Cardiothoracic Surgery, Stanford University, London, UK
| | - Peter Kohl
- National Heart and Lung Institute, Imperial College, London, UK
| | | | | | - Stephen Large
- Department of Cardiothoracic Surgery, Papworth Hospital, Cambridge, UK
| | - Ziad Ali
- Division of Cardiology, Columbia University, New York, NY
| | - Euan Ashley
- Division of Cardiovascular Medicine, Stanford University, Stanford, CA
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de Tombe PP, Kohl P. Which way to grow? Force over time may be the heart's Dao de jing. Glob Cardiol Sci Pract 2016; 2016:e201621. [PMID: 29043268 PMCID: PMC5642831 DOI: 10.21542/gcsp.2016.21] [Citation(s) in RCA: 0] [Impact Index Per Article: 0] [Reference Citation Analysis] [Track Full Text] [Download PDF] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Indexed: 11/24/2022] Open
Affiliation(s)
- Pieter P de Tombe
- Department of Cell and Molecular Physiology, Loyola University Chicago, Stritch School of Medicine, Maywood, IL 60304, USA
| | - Peter Kohl
- Cardiac Biophysics and Systems Biology, National Heart and Lung Institute, Imperial College London, UK.,Institute for Experimental Cardiovascular Medicine, University Heart Centre Freiburg - Bad Krozingen, and Faculty of Medicine, Albert Ludwigs University Freiburg, Germany
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33
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Lichter J, Li H, Sachse FB. Measurement of Strain in Cardiac Myocytes at Micrometer Scale Based on Rapid Scanning Confocal Microscopy and Non-Rigid Image Registration. Ann Biomed Eng 2016; 44:3020-3031. [PMID: 27001400 DOI: 10.1007/s10439-016-1593-7] [Citation(s) in RCA: 3] [Impact Index Per Article: 0.4] [Reference Citation Analysis] [Abstract] [Key Words] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Received: 12/03/2015] [Accepted: 03/12/2016] [Indexed: 12/17/2022]
Abstract
Measurement of cell shortening is an important technique for assessment of physiology and pathophysiology of cardiac myocytes. Many types of heart disease are associated with decreased myocyte shortening, which is commonly caused by structural and functional remodeling. Here, we present a new approach for local measurement of 2-dimensional strain within cells at high spatial resolution. The approach applies non-rigid image registration to quantify local displacements and Cauchy strain in images of cells undergoing contraction. We extensively evaluated the approach using synthetic cell images and image sequences from rapid scanning confocal microscopy of fluorescently labeled isolated myocytes from the left ventricle of normal and diseased canine heart. Application of the approach yielded a comprehensive description of cellular strain including novel measurements of transverse strain and spatial heterogeneity of strain. Quantitative comparison with manual measurements of strain in image sequences indicated reliability of the developed approach. We suggest that the developed approach provides researchers with a novel tool to investigate contractility of cardiac myocytes at subcellular scale. In contrast to previously introduced methods for measuring cell shorting, the developed approach provides comprehensive information on the spatio-temporal distribution of 2-dimensional strain at micrometer scale.
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Affiliation(s)
- J Lichter
- Nora Eccles Harrison Cardiovascular Research and Training Institute, University of Utah, 95 South 2000 East, Salt Lake City, UT, 84112-5000, USA.,Department of Bioengineering, University of Utah, Salt Lake City, UT, 84112, USA
| | - Hui Li
- Nora Eccles Harrison Cardiovascular Research and Training Institute, University of Utah, 95 South 2000 East, Salt Lake City, UT, 84112-5000, USA
| | - Frank B Sachse
- Nora Eccles Harrison Cardiovascular Research and Training Institute, University of Utah, 95 South 2000 East, Salt Lake City, UT, 84112-5000, USA. .,Department of Bioengineering, University of Utah, Salt Lake City, UT, 84112, USA.
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Awasthi S, Izu LT, Mao Z, Jian Z, Landas T, Lerner A, Shimkunas R, Woldeyesus R, Bossuyt J, Wood BM, Chen YJ, Matthews DL, Lieu DK, Chiamvimonvat N, Lam KS, Chen-Izu Y, Chan JW. Multimodal SHG-2PF Imaging of Microdomain Ca2+-Contraction Coupling in Live Cardiac Myocytes. Circ Res 2015; 118:e19-28. [PMID: 26643875 DOI: 10.1161/circresaha.115.307919] [Citation(s) in RCA: 17] [Impact Index Per Article: 1.9] [Reference Citation Analysis] [Abstract] [Key Words] [Track Full Text] [Journal Information] [Submit a Manuscript] [Subscribe] [Scholar Register] [Received: 11/06/2015] [Accepted: 12/07/2015] [Indexed: 01/24/2023]
Abstract
RATIONALE Cardiac myocyte contraction is caused by Ca(2+) binding to troponin C, which triggers the cross-bridge power stroke and myofilament sliding in sarcomeres. Synchronized Ca(2+) release causes whole cell contraction and is readily observable with current microscopy techniques. However, it is unknown whether localized Ca(2+) release, such as Ca(2+) sparks and waves, can cause local sarcomere contraction. Contemporary imaging methods fall short of measuring microdomain Ca(2+)-contraction coupling in live cardiac myocytes. OBJECTIVE To develop a method for imaging sarcomere level Ca(2+)-contraction coupling in healthy and disease model cardiac myocytes. METHODS AND RESULTS Freshly isolated cardiac myocytes were loaded with the Ca(2+)-indicator fluo-4. A confocal microscope equipped with a femtosecond-pulsed near-infrared laser was used to simultaneously excite second harmonic generation from A-bands of myofibrils and 2-photon fluorescence from fluo-4. Ca(2+) signals and sarcomere strain correlated in space and time with short delays. Furthermore, Ca(2+) sparks and waves caused contractions in subcellular microdomains, revealing a previously underappreciated role for these events in generating subcellular strain during diastole. Ca(2+) activity and sarcomere strain were also imaged in paced cardiac myocytes under mechanical load, revealing spontaneous Ca(2+) waves and correlated local contraction in pressure-overload-induced cardiomyopathy. CONCLUSIONS Multimodal second harmonic generation 2-photon fluorescence microscopy enables the simultaneous observation of Ca(2+) release and mechanical strain at the subsarcomere level in living cardiac myocytes. The method benefits from the label-free nature of second harmonic generation, which allows A-bands to be imaged independently of T-tubule morphology and simultaneously with Ca(2+) indicators. Second harmonic generation 2-photon fluorescence imaging is widely applicable to the study of Ca(2+)-contraction coupling and mechanochemotransduction in both health and disease.
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Affiliation(s)
- Samir Awasthi
- From the Center for Biophotonics (S.A., Z.M., A.L., D.L.M., J.W.C.), Division of Cardiology (D.K.L., N.C., Y.C.-I.), Division of Hematology/Oncology, Department of Internal Medicine (K.S.L.), and Department of Pathology and Laboratory Medicine (J.W.C.), UC Davis School of Medicine, University of California, Davis, Sacramento; and Departments of Pharmacology (L.T.I., Z.J., T.L., J.B., B.W., Y.-J.C., Y.C.-I.), Biomedical Engineering (S.A., R.S., R.W., Y.C.-I.), Biochemistry and Molecular Medicine (K.S.L.), and Microsurgery Core (Y.-J.C.), University of California, Davis
| | - Leighton T Izu
- From the Center for Biophotonics (S.A., Z.M., A.L., D.L.M., J.W.C.), Division of Cardiology (D.K.L., N.C., Y.C.-I.), Division of Hematology/Oncology, Department of Internal Medicine (K.S.L.), and Department of Pathology and Laboratory Medicine (J.W.C.), UC Davis School of Medicine, University of California, Davis, Sacramento; and Departments of Pharmacology (L.T.I., Z.J., T.L., J.B., B.W., Y.-J.C., Y.C.-I.), Biomedical Engineering (S.A., R.S., R.W., Y.C.-I.), Biochemistry and Molecular Medicine (K.S.L.), and Microsurgery Core (Y.-J.C.), University of California, Davis
| | - Ziliang Mao
- From the Center for Biophotonics (S.A., Z.M., A.L., D.L.M., J.W.C.), Division of Cardiology (D.K.L., N.C., Y.C.-I.), Division of Hematology/Oncology, Department of Internal Medicine (K.S.L.), and Department of Pathology and Laboratory Medicine (J.W.C.), UC Davis School of Medicine, University of California, Davis, Sacramento; and Departments of Pharmacology (L.T.I., Z.J., T.L., J.B., B.W., Y.-J.C., Y.C.-I.), Biomedical Engineering (S.A., R.S., R.W., Y.C.-I.), Biochemistry and Molecular Medicine (K.S.L.), and Microsurgery Core (Y.-J.C.), University of California, Davis
| | - Zhong Jian
- From the Center for Biophotonics (S.A., Z.M., A.L., D.L.M., J.W.C.), Division of Cardiology (D.K.L., N.C., Y.C.-I.), Division of Hematology/Oncology, Department of Internal Medicine (K.S.L.), and Department of Pathology and Laboratory Medicine (J.W.C.), UC Davis School of Medicine, University of California, Davis, Sacramento; and Departments of Pharmacology (L.T.I., Z.J., T.L., J.B., B.W., Y.-J.C., Y.C.-I.), Biomedical Engineering (S.A., R.S., R.W., Y.C.-I.), Biochemistry and Molecular Medicine (K.S.L.), and Microsurgery Core (Y.-J.C.), University of California, Davis
| | - Trevor Landas
- From the Center for Biophotonics (S.A., Z.M., A.L., D.L.M., J.W.C.), Division of Cardiology (D.K.L., N.C., Y.C.-I.), Division of Hematology/Oncology, Department of Internal Medicine (K.S.L.), and Department of Pathology and Laboratory Medicine (J.W.C.), UC Davis School of Medicine, University of California, Davis, Sacramento; and Departments of Pharmacology (L.T.I., Z.J., T.L., J.B., B.W., Y.-J.C., Y.C.-I.), Biomedical Engineering (S.A., R.S., R.W., Y.C.-I.), Biochemistry and Molecular Medicine (K.S.L.), and Microsurgery Core (Y.-J.C.), University of California, Davis
| | - Aaron Lerner
- From the Center for Biophotonics (S.A., Z.M., A.L., D.L.M., J.W.C.), Division of Cardiology (D.K.L., N.C., Y.C.-I.), Division of Hematology/Oncology, Department of Internal Medicine (K.S.L.), and Department of Pathology and Laboratory Medicine (J.W.C.), UC Davis School of Medicine, University of California, Davis, Sacramento; and Departments of Pharmacology (L.T.I., Z.J., T.L., J.B., B.W., Y.-J.C., Y.C.-I.), Biomedical Engineering (S.A., R.S., R.W., Y.C.-I.), Biochemistry and Molecular Medicine (K.S.L.), and Microsurgery Core (Y.-J.C.), University of California, Davis
| | - Rafael Shimkunas
- From the Center for Biophotonics (S.A., Z.M., A.L., D.L.M., J.W.C.), Division of Cardiology (D.K.L., N.C., Y.C.-I.), Division of Hematology/Oncology, Department of Internal Medicine (K.S.L.), and Department of Pathology and Laboratory Medicine (J.W.C.), UC Davis School of Medicine, University of California, Davis, Sacramento; and Departments of Pharmacology (L.T.I., Z.J., T.L., J.B., B.W., Y.-J.C., Y.C.-I.), Biomedical Engineering (S.A., R.S., R.W., Y.C.-I.), Biochemistry and Molecular Medicine (K.S.L.), and Microsurgery Core (Y.-J.C.), University of California, Davis
| | - Rahwa Woldeyesus
- From the Center for Biophotonics (S.A., Z.M., A.L., D.L.M., J.W.C.), Division of Cardiology (D.K.L., N.C., Y.C.-I.), Division of Hematology/Oncology, Department of Internal Medicine (K.S.L.), and Department of Pathology and Laboratory Medicine (J.W.C.), UC Davis School of Medicine, University of California, Davis, Sacramento; and Departments of Pharmacology (L.T.I., Z.J., T.L., J.B., B.W., Y.-J.C., Y.C.-I.), Biomedical Engineering (S.A., R.S., R.W., Y.C.-I.), Biochemistry and Molecular Medicine (K.S.L.), and Microsurgery Core (Y.-J.C.), University of California, Davis
| | - Julie Bossuyt
- From the Center for Biophotonics (S.A., Z.M., A.L., D.L.M., J.W.C.), Division of Cardiology (D.K.L., N.C., Y.C.-I.), Division of Hematology/Oncology, Department of Internal Medicine (K.S.L.), and Department of Pathology and Laboratory Medicine (J.W.C.), UC Davis School of Medicine, University of California, Davis, Sacramento; and Departments of Pharmacology (L.T.I., Z.J., T.L., J.B., B.W., Y.-J.C., Y.C.-I.), Biomedical Engineering (S.A., R.S., R.W., Y.C.-I.), Biochemistry and Molecular Medicine (K.S.L.), and Microsurgery Core (Y.-J.C.), University of California, Davis
| | - Brent M Wood
- From the Center for Biophotonics (S.A., Z.M., A.L., D.L.M., J.W.C.), Division of Cardiology (D.K.L., N.C., Y.C.-I.), Division of Hematology/Oncology, Department of Internal Medicine (K.S.L.), and Department of Pathology and Laboratory Medicine (J.W.C.), UC Davis School of Medicine, University of California, Davis, Sacramento; and Departments of Pharmacology (L.T.I., Z.J., T.L., J.B., B.W., Y.-J.C., Y.C.-I.), Biomedical Engineering (S.A., R.S., R.W., Y.C.-I.), Biochemistry and Molecular Medicine (K.S.L.), and Microsurgery Core (Y.-J.C.), University of California, Davis
| | - Yi-Je Chen
- From the Center for Biophotonics (S.A., Z.M., A.L., D.L.M., J.W.C.), Division of Cardiology (D.K.L., N.C., Y.C.-I.), Division of Hematology/Oncology, Department of Internal Medicine (K.S.L.), and Department of Pathology and Laboratory Medicine (J.W.C.), UC Davis School of Medicine, University of California, Davis, Sacramento; and Departments of Pharmacology (L.T.I., Z.J., T.L., J.B., B.W., Y.-J.C., Y.C.-I.), Biomedical Engineering (S.A., R.S., R.W., Y.C.-I.), Biochemistry and Molecular Medicine (K.S.L.), and Microsurgery Core (Y.-J.C.), University of California, Davis
| | - Dennis L Matthews
- From the Center for Biophotonics (S.A., Z.M., A.L., D.L.M., J.W.C.), Division of Cardiology (D.K.L., N.C., Y.C.-I.), Division of Hematology/Oncology, Department of Internal Medicine (K.S.L.), and Department of Pathology and Laboratory Medicine (J.W.C.), UC Davis School of Medicine, University of California, Davis, Sacramento; and Departments of Pharmacology (L.T.I., Z.J., T.L., J.B., B.W., Y.-J.C., Y.C.-I.), Biomedical Engineering (S.A., R.S., R.W., Y.C.-I.), Biochemistry and Molecular Medicine (K.S.L.), and Microsurgery Core (Y.-J.C.), University of California, Davis
| | - Deborah K Lieu
- From the Center for Biophotonics (S.A., Z.M., A.L., D.L.M., J.W.C.), Division of Cardiology (D.K.L., N.C., Y.C.-I.), Division of Hematology/Oncology, Department of Internal Medicine (K.S.L.), and Department of Pathology and Laboratory Medicine (J.W.C.), UC Davis School of Medicine, University of California, Davis, Sacramento; and Departments of Pharmacology (L.T.I., Z.J., T.L., J.B., B.W., Y.-J.C., Y.C.-I.), Biomedical Engineering (S.A., R.S., R.W., Y.C.-I.), Biochemistry and Molecular Medicine (K.S.L.), and Microsurgery Core (Y.-J.C.), University of California, Davis
| | - Nipavan Chiamvimonvat
- From the Center for Biophotonics (S.A., Z.M., A.L., D.L.M., J.W.C.), Division of Cardiology (D.K.L., N.C., Y.C.-I.), Division of Hematology/Oncology, Department of Internal Medicine (K.S.L.), and Department of Pathology and Laboratory Medicine (J.W.C.), UC Davis School of Medicine, University of California, Davis, Sacramento; and Departments of Pharmacology (L.T.I., Z.J., T.L., J.B., B.W., Y.-J.C., Y.C.-I.), Biomedical Engineering (S.A., R.S., R.W., Y.C.-I.), Biochemistry and Molecular Medicine (K.S.L.), and Microsurgery Core (Y.-J.C.), University of California, Davis
| | - Kit S Lam
- From the Center for Biophotonics (S.A., Z.M., A.L., D.L.M., J.W.C.), Division of Cardiology (D.K.L., N.C., Y.C.-I.), Division of Hematology/Oncology, Department of Internal Medicine (K.S.L.), and Department of Pathology and Laboratory Medicine (J.W.C.), UC Davis School of Medicine, University of California, Davis, Sacramento; and Departments of Pharmacology (L.T.I., Z.J., T.L., J.B., B.W., Y.-J.C., Y.C.-I.), Biomedical Engineering (S.A., R.S., R.W., Y.C.-I.), Biochemistry and Molecular Medicine (K.S.L.), and Microsurgery Core (Y.-J.C.), University of California, Davis
| | - Ye Chen-Izu
- From the Center for Biophotonics (S.A., Z.M., A.L., D.L.M., J.W.C.), Division of Cardiology (D.K.L., N.C., Y.C.-I.), Division of Hematology/Oncology, Department of Internal Medicine (K.S.L.), and Department of Pathology and Laboratory Medicine (J.W.C.), UC Davis School of Medicine, University of California, Davis, Sacramento; and Departments of Pharmacology (L.T.I., Z.J., T.L., J.B., B.W., Y.-J.C., Y.C.-I.), Biomedical Engineering (S.A., R.S., R.W., Y.C.-I.), Biochemistry and Molecular Medicine (K.S.L.), and Microsurgery Core (Y.-J.C.), University of California, Davis.
| | - James W Chan
- From the Center for Biophotonics (S.A., Z.M., A.L., D.L.M., J.W.C.), Division of Cardiology (D.K.L., N.C., Y.C.-I.), Division of Hematology/Oncology, Department of Internal Medicine (K.S.L.), and Department of Pathology and Laboratory Medicine (J.W.C.), UC Davis School of Medicine, University of California, Davis, Sacramento; and Departments of Pharmacology (L.T.I., Z.J., T.L., J.B., B.W., Y.-J.C., Y.C.-I.), Biomedical Engineering (S.A., R.S., R.W., Y.C.-I.), Biochemistry and Molecular Medicine (K.S.L.), and Microsurgery Core (Y.-J.C.), University of California, Davis.
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Kijlstra JD, Hu D, Mittal N, Kausel E, van der Meer P, Garakani A, Domian IJ. Integrated Analysis of Contractile Kinetics, Force Generation, and Electrical Activity in Single Human Stem Cell-Derived Cardiomyocytes. Stem Cell Reports 2015; 5:1226-1238. [PMID: 26626178 PMCID: PMC4682285 DOI: 10.1016/j.stemcr.2015.10.017] [Citation(s) in RCA: 50] [Impact Index Per Article: 5.6] [Reference Citation Analysis] [Abstract] [Track Full Text] [Download PDF] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Received: 04/02/2015] [Revised: 10/28/2015] [Accepted: 10/29/2015] [Indexed: 10/25/2022] Open
Abstract
The quantitative analysis of cardiomyocyte function is essential for stem cell-based approaches for the in vitro study of human cardiac physiology and pathophysiology. We present a method to comprehensively assess the function of single human pluripotent stem cell-derived cardiomyocyte (hPSC-CMs) through simultaneous quantitative analysis of contraction kinetics, force generation, and electrical activity. We demonstrate that statistical analysis of movies of contracting hPSC-CMs can be used to quantify changes in cellular morphology over time and compute contractile kinetics. Using a biomechanical model that incorporates substrate stiffness, we calculate cardiomyocyte force generation at single-cell resolution and validate this approach with conventional traction force microscopy. The addition of fluorescent calcium indicators or membrane potential dyes allows the simultaneous analysis of contractility and calcium handling or action potential morphology. Accordingly, our approach has the potential for broad application in the study of cardiac disease, drug discovery, and cardiotoxicity screening.
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Affiliation(s)
- Jan David Kijlstra
- Cardiovascular Research Center, Massachusetts General Hospital, Boston, MA 02114, USA; Harvard Medical School, Boston, MA 02115, USA; University Medical Center Groningen, University of Groningen, Groningen, 9713 GZ, the Netherlands
| | - Dongjian Hu
- Cardiovascular Research Center, Massachusetts General Hospital, Boston, MA 02114, USA; Harvard Medical School, Boston, MA 02115, USA; Department of Biomedical Engineering, Boston University, Boston, MA 02215, USA
| | - Nikhil Mittal
- Institute of Bioengineering and Nanotechnology, 138669 Singapore
| | - Eduardo Kausel
- Department of Civil and Environmental Engineering, Massachusetts Institute of Technology, Cambridge, MA 02139, USA
| | - Peter van der Meer
- University Medical Center Groningen, University of Groningen, Groningen, 9713 GZ, the Netherlands
| | | | - Ibrahim J Domian
- Cardiovascular Research Center, Massachusetts General Hospital, Boston, MA 02114, USA; Harvard Medical School, Boston, MA 02115, USA; Harvard Stem Cell Institute, Cambridge, MA 02138, USA.
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Abstract
Real-time microscopic imaging of moving organs at single-cell resolution represents a major challenge in studying complex biology in living systems. Motion of the tissue from the cardiac and respiratory cycles severely limits intravital microscopy by compromising ultimate spatial and temporal imaging resolution. However, significant recent advances have enabled single-cell resolution imaging to be achieved in vivo. In this protocol, we describe experimental procedures for intravital microscopy based on a combination of thoracic surgery, tissue stabilizers and acquisition gating methods, which enable imaging at the single-cell level in the beating heart in the mouse. Setup of the model is typically completed in 1 h, which allows 2 h or more of continuous cardiac imaging. This protocol can be readily adapted for the imaging of other moving organs, and it will therefore broadly facilitate in vivo high-resolution microscopy studies.
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Nance ME, Whitfield JT, Zhu Y, Gibson AK, Hanft LM, Campbell KS, Meininger GA, McDonald KS, Segal SS, Domeier TL. Attenuated sarcomere lengthening of the aged murine left ventricle observed using two-photon fluorescence microscopy. Am J Physiol Heart Circ Physiol 2015. [PMID: 26209054 DOI: 10.1152/ajpheart.00315.2015] [Citation(s) in RCA: 12] [Impact Index Per Article: 1.3] [Reference Citation Analysis] [Abstract] [Key Words] [Track Full Text] [Journal Information] [Submit a Manuscript] [Subscribe] [Scholar Register] [Indexed: 12/25/2022]
Abstract
The Frank-Starling mechanism, whereby increased diastolic filling leads to increased cardiac output, depends on increasing the sarcomere length (Ls) of cardiomyocytes. Ventricular stiffness increases with advancing age, yet it remains unclear how such changes in compliance impact sarcomere dynamics in the intact heart. We developed an isolated murine heart preparation to monitor Ls as a function of left ventricular pressure and tested the hypothesis that sarcomere lengthening in response to ventricular filling is impaired with advanced age. Mouse hearts isolated from young (3-6 mo) and aged (24-28 mo) C57BL/6 mice were perfused via the aorta under Ca(2+)-free conditions with the left ventricle cannulated to control filling pressure. Two-photon imaging of 4-{2-[6-(dioctylamino)-2-naphthalenyl]ethenyl}1-(3-sulfopropyl)-pyridinium fluorescence was used to monitor t-tubule striations and obtain passive Ls between pressures of 0 and 40 mmHg. Ls values (in μm, aged vs. young, respectively) were 2.02 ± 0.04 versus 2.01 ± 0.02 at 0 mmHg, 2.13 ± 0.04 versus 2.23 ± 0.02 at 5 mmHg, 2.21 ± 0.03 versus 2.27 ± 0.03 at 10 mmHg, and 2.28 ± 0.02 versus 2.36 ± 0.01 at 40 mmHg, indicative of impaired sarcomere lengthening in aged hearts. Atomic force microscopy nanoindentation revealed that intact cardiomyocytes enzymatically isolated from aged hearts had increased stiffness compared with those of young hearts (elastic modulus: aged, 41.9 ± 5.8 kPa vs. young, 18.6 ± 3.3 kPa; P = 0.006). Impaired sarcomere lengthening during left ventricular filling may contribute to cardiac dysfunction with advancing age by attenuating the Frank-Starling mechanism and reducing stroke volume.
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Affiliation(s)
- Michael E Nance
- Molecular Pathogenesis and Therapeutics Graduate Program, University of Missouri School of Medicine, Columbia, Missouri
| | - Justin T Whitfield
- Department of Medical Pharmacology and Physiology, University of Missouri School of Medicine, Columbia, Missouri
| | - Yi Zhu
- Department of Medical Pharmacology and Physiology, University of Missouri School of Medicine, Columbia, Missouri
| | - Anne K Gibson
- Department of Medical Pharmacology and Physiology, University of Missouri School of Medicine, Columbia, Missouri
| | - Laurin M Hanft
- Department of Medical Pharmacology and Physiology, University of Missouri School of Medicine, Columbia, Missouri
| | - Kenneth S Campbell
- Department of Physiology, University of Kentucky College of Medicine, Lexington, Kentucky
| | - Gerald A Meininger
- Department of Medical Pharmacology and Physiology, University of Missouri School of Medicine, Columbia, Missouri; Dalton Cardiovascular Research Center, University of Missouri, Columbia, Missouri; and
| | - Kerry S McDonald
- Department of Medical Pharmacology and Physiology, University of Missouri School of Medicine, Columbia, Missouri
| | - Steven S Segal
- Department of Medical Pharmacology and Physiology, University of Missouri School of Medicine, Columbia, Missouri; Dalton Cardiovascular Research Center, University of Missouri, Columbia, Missouri; and
| | - Timothy L Domeier
- Department of Medical Pharmacology and Physiology, University of Missouri School of Medicine, Columbia, Missouri;
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Fowler ED, Benoist D, Drinkhill MJ, Stones R, Helmes M, Wüst RCI, Stienen GJM, Steele DS, White E. Decreased creatine kinase is linked to diastolic dysfunction in rats with right heart failure induced by pulmonary artery hypertension. J Mol Cell Cardiol 2015; 86:1-8. [PMID: 26116865 PMCID: PMC4564291 DOI: 10.1016/j.yjmcc.2015.06.016] [Citation(s) in RCA: 39] [Impact Index Per Article: 4.3] [Reference Citation Analysis] [Abstract] [Key Words] [MESH Headings] [Grants] [Download PDF] [Figures] [Journal Information] [Submit a Manuscript] [Subscribe] [Scholar Register] [Received: 11/26/2014] [Revised: 06/19/2015] [Accepted: 06/22/2015] [Indexed: 02/01/2023]
Abstract
Our objective was to investigate the role of creatine kinase in the contractile dysfunction of right ventricular failure caused by pulmonary artery hypertension. Pulmonary artery hypertension and right ventricular failure were induced in rats by monocrotaline and compared to saline-injected control animals. In vivo right ventricular diastolic pressure-volume relationships were measured in anesthetized animals; diastolic force-length relationships in single enzymatically dissociated myocytes and myocardial creatine kinase levels by Western blot. We observed diastolic dysfunction in right ventricular failure indicated by significantly steeper diastolic pressure-volume relationships in vivo and diastolic force-length relationships in single myocytes. There was a significant reduction in creatine kinase protein expression in failing right ventricle. Dysfunction also manifested as a shorter diastolic sarcomere length in failing myocytes. This was associated with a Ca(2+)-independent mechanism that was sensitive to cross-bridge cycling inhibition. In saponin-skinned failing myocytes, addition of exogenous creatine kinase significantly lengthened sarcomeres, while in intact healthy myocytes, inhibition of creatine kinase significantly shortened sarcomeres. Creatine kinase inhibition also changed the relatively flat contraction amplitude-stimulation frequency relationship of healthy myocytes into a steeply negative, failing phenotype. Decreased creatine kinase expression leads to diastolic dysfunction. We propose that this is via local reduction in ATP:ADP ratio and thus to Ca(2+)-independent force production and diastolic sarcomere shortening. Creatine kinase inhibition also mimics a definitive characteristic of heart failure, the inability to respond to increased demand. Novel therapies for pulmonary artery hypertension are needed. Our data suggest that cardiac energetics would be a potential ventricular therapeutic target.
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Affiliation(s)
- Ewan D Fowler
- Multidisciplinary Cardiovascular Research Centre, University of Leeds, UK
| | - David Benoist
- Multidisciplinary Cardiovascular Research Centre, University of Leeds, UK; L'Institut de Rythmologie et Modélisation Cardiaque, Inserm U-1045, Université de Bordeaux, France
| | - Mark J Drinkhill
- Multidisciplinary Cardiovascular Research Centre, University of Leeds, UK
| | - Rachel Stones
- Multidisciplinary Cardiovascular Research Centre, University of Leeds, UK
| | - Michiel Helmes
- Department of Physiology, Institute for Cardiovascular Research, VU University Medical Centre, Amsterdam, The Netherlands; IonOptix LLC, Milton, MA, USA
| | - Rob C I Wüst
- Department of Physiology, Institute for Cardiovascular Research, VU University Medical Centre, Amsterdam, The Netherlands
| | - Ger J M Stienen
- Department of Physiology, Institute for Cardiovascular Research, VU University Medical Centre, Amsterdam, The Netherlands; Department of Physics and Astronomy, Faculty of Science, VU University, Amsterdam, The Netherlands
| | - Derek S Steele
- Multidisciplinary Cardiovascular Research Centre, University of Leeds, UK
| | - Ed White
- Multidisciplinary Cardiovascular Research Centre, University of Leeds, UK.
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Tan Y, Richards D, Xu R, Stewart-Clark S, Mani SK, Borg TK, Menick DR, Tian B, Mei Y. Silicon nanowire-induced maturation of cardiomyocytes derived from human induced pluripotent stem cells. NANO LETTERS 2015; 15:2765-72. [PMID: 25826336 PMCID: PMC4431939 DOI: 10.1021/nl502227a] [Citation(s) in RCA: 58] [Impact Index Per Article: 6.4] [Reference Citation Analysis] [Abstract] [Key Words] [MESH Headings] [Grants] [Track Full Text] [Subscribe] [Scholar Register] [Indexed: 05/10/2023]
Abstract
The current inability to derive mature cardiomyocytes from human pluripotent stem cells has been the limiting step for transitioning this powerful technology into clinical therapies. To address this, scaffold-based tissue engineering approaches have been utilized to mimic heart development in vitro and promote maturation of cardiomyocytes derived from human pluripotent stem cells. While scaffolds can provide 3D microenvironments, current scaffolds lack the matched physical/chemical/biological properties of native extracellular environments. On the other hand, scaffold-free, 3D cardiac spheroids (i.e., spherical-shaped microtissues) prepared by seeding cardiomyocytes into agarose microwells were shown to improve cardiac functions. However, cardiomyocytes within the spheroids could not assemble in a controlled manner and led to compromised, unsynchronized contractions. Here, we show, for the first time, that incorporation of a trace amount (i.e., ∼0.004% w/v) of electrically conductive silicon nanowires (e-SiNWs) in otherwise scaffold-free cardiac spheroids can form an electrically conductive network, leading to synchronized and significantly enhanced contraction (i.e., >55% increase in average contraction amplitude), resulting in significantly more advanced cellular structural and contractile maturation.
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Affiliation(s)
- Yu Tan
- Bioengineering Department, Clemson University, Clemson, SC 29634, USA
| | - Dylan Richards
- Bioengineering Department, Clemson University, Clemson, SC 29634, USA
| | - Ruoyu Xu
- Department of Chemistry, the James Franck Institute and the Institute for Biophysical Dynamics, the University of Chicago, Chicago, IL 60637, USA
| | | | - Santhosh Kumar Mani
- Division of Cardiology, Department of Medicine, Gazes Cardiac Research Institute, Medical University of South Carolina, Charleston SC 29425, USA
| | - Thomas Keith Borg
- Bioengineering Department, Clemson University, Clemson, SC 29634, USA
- Department of Regenerative Medicine and Cell Biology, Medical University of South Carolina, Charleston, SC 29425, USA
| | - Donald R. Menick
- Division of Cardiology, Department of Medicine, Gazes Cardiac Research Institute, Medical University of South Carolina, Charleston SC 29425, USA
| | - Bozhi Tian
- Department of Chemistry, the James Franck Institute and the Institute for Biophysical Dynamics, the University of Chicago, Chicago, IL 60637, USA
| | - Ying Mei
- Bioengineering Department, Clemson University, Clemson, SC 29634, USA
- Department of Regenerative Medicine and Cell Biology, Medical University of South Carolina, Charleston, SC 29425, USA
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Corbett AD, Burton RAB, Bub G, Salter PS, Tuohy S, Booth MJ, Wilson T. Quantifying distortions in two-photon remote focussing microscope images using a volumetric calibration specimen. Front Physiol 2014; 5:384. [PMID: 25339910 PMCID: PMC4189333 DOI: 10.3389/fphys.2014.00384] [Citation(s) in RCA: 9] [Impact Index Per Article: 0.9] [Reference Citation Analysis] [Abstract] [Key Words] [Track Full Text] [Download PDF] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Received: 06/27/2014] [Accepted: 09/18/2014] [Indexed: 02/03/2023] Open
Abstract
Remote focussing microscopy allows sharp, in-focus images to be acquired at high speed from outside of the focal plane of an objective lens without any agitation of the specimen. However, without careful optical alignment, the advantages of remote focussing microscopy could be compromised by the introduction of depth-dependent scaling artifacts. To achieve an ideal alignment in a point-scanning remote focussing microscope, the lateral (XY) scan mirror pair must be imaged onto the back focal plane of both the reference and imaging objectives, in a telecentric arrangement. However, for many commercial objective lenses, it can be difficult to accurately locate the position of the back focal plane. This paper investigates the impact of this limitation on the fidelity of three-dimensional data sets of living cardiac tissue, specifically the introduction of distortions. These distortions limit the accuracy of sarcomere measurements taken directly from raw volumetric data. The origin of the distortion is first identified through simulation of a remote focussing microscope. Using a novel three-dimensional calibration specimen it was then possible to quantify experimentally the size of the distortion as a function of objective misalignment. Finally, by first approximating and then compensating the distortion in imaging data from whole heart rodent studies, the variance of sarcomere length (SL) measurements was reduced by almost 50%.
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Affiliation(s)
- Alexander D Corbett
- Department of Engineering Science, University of Oxford Oxford, UK ; Department of Physiology, Anatomy and Genetics, University of Oxford Oxford, UK
| | - Rebecca A B Burton
- Department of Physiology, Anatomy and Genetics, University of Oxford Oxford, UK
| | - Gil Bub
- Department of Physiology, Anatomy and Genetics, University of Oxford Oxford, UK
| | - Patrick S Salter
- Department of Engineering Science, University of Oxford Oxford, UK
| | - Simon Tuohy
- Department of Physiology, Anatomy and Genetics, University of Oxford Oxford, UK
| | - Martin J Booth
- Department of Engineering Science, University of Oxford Oxford, UK ; Department of Physiology, Anatomy and Genetics, University of Oxford Oxford, UK
| | - Tony Wilson
- Department of Engineering Science, University of Oxford Oxford, UK
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Images as drivers of progress in cardiac computational modelling. PROGRESS IN BIOPHYSICS AND MOLECULAR BIOLOGY 2014; 115:198-212. [PMID: 25117497 PMCID: PMC4210662 DOI: 10.1016/j.pbiomolbio.2014.08.005] [Citation(s) in RCA: 40] [Impact Index Per Article: 4.0] [Reference Citation Analysis] [Abstract] [Key Words] [Track Full Text] [Download PDF] [Figures] [Subscribe] [Scholar Register] [Received: 07/24/2014] [Accepted: 08/02/2014] [Indexed: 11/28/2022]
Abstract
Computational models have become a fundamental tool in cardiac research. Models are evolving to cover multiple scales and physical mechanisms. They are moving towards mechanistic descriptions of personalised structure and function, including effects of natural variability. These developments are underpinned to a large extent by advances in imaging technologies. This article reviews how novel imaging technologies, or the innovative use and extension of established ones, integrate with computational models and drive novel insights into cardiac biophysics. In terms of structural characterization, we discuss how imaging is allowing a wide range of scales to be considered, from cellular levels to whole organs. We analyse how the evolution from structural to functional imaging is opening new avenues for computational models, and in this respect we review methods for measurement of electrical activity, mechanics and flow. Finally, we consider ways in which combined imaging and modelling research is likely to continue advancing cardiac research, and identify some of the main challenges that remain to be solved.
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42
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Lohezic M, Teh I, Bollensdorff C, Peyronnet R, Hales PW, Grau V, Kohl P, Schneider JE. Interrogation of living myocardium in multiple static deformation states with diffusion tensor and diffusion spectrum imaging. PROGRESS IN BIOPHYSICS AND MOLECULAR BIOLOGY 2014; 115:213-25. [PMID: 25117498 PMCID: PMC4210665 DOI: 10.1016/j.pbiomolbio.2014.08.002] [Citation(s) in RCA: 17] [Impact Index Per Article: 1.7] [Reference Citation Analysis] [Abstract] [Key Words] [Track Full Text] [Figures] [Subscribe] [Scholar Register] [Received: 07/22/2014] [Accepted: 08/02/2014] [Indexed: 11/27/2022]
Abstract
Diffusion tensor magnetic resonance imaging (MRI) reveals valuable insights into tissue histo-anatomy and microstructure, and has steadily gained traction in the cardiac community. Its wider use in small animal cardiac imaging in vivo has been constrained by its extreme sensitivity to motion, exaggerated by the high heart rates usually seen in rodents. Imaging of the isolated heart eliminates respiratory motion and, if conducted on arrested hearts, cardiac pulsation. This serves as an important intermediate step for basic and translational studies. However, investigating the micro-structural basis of cardiac deformation in the same heart requires observations in different deformation states. Here, we illustrate the imaging of isolated rat hearts in three mechanical states mimicking diastole (cardioplegic arrest), left-ventricular (LV) volume overload (cardioplegic arrest plus LV balloon inflation), and peak systole (lithium-induced contracture). An optimised MRI-compatible Langendorff perfusion setup with the radio-frequency (RF) coil integrated into the wet chamber was developed for use in a 9.4T horizontal bore scanner. Signal-to-noise ratio improved significantly, by 75% compared to a previous design with external RF coil, and stability tests showed no significant changes in mean T1, T2 or LV wall thickness over a 170 min period. In contracture, we observed a significant reduction in mean fractional anisotropy from 0.32 ± 0.02 to 0.28 ± 0.02, as well as a significant rightward shift in helix angles with a decrease in the proportion of left-handed fibres, as referring to the locally prevailing cell orientation in the heart, from 24.9% to 23.3%, and an increase in the proportion of right-handed fibres from 25.5% to 28.4%. LV overload, in contrast, gave rise to a decrease in the proportion of left-handed fibres from 24.9% to 21.4% and an increase in the proportion of right-handed fibres from 25.5% to 26.0%. The modified perfusion and coil setup offers better performance and control over cardiac contraction states. We subsequently performed high-resolution diffusion spectrum imaging (DSI) and 3D whole heart fibre tracking in fixed ex vivo rat hearts in slack state and contracture. As a model-free method, DSI augmented the measurements of water diffusion by also informing on multiple intra-voxel diffusion orientations and non-Gaussian diffusion. This enabled us to identify the transition from right- to left-handed fibres from the subendocardium to the subepicardium, as well as voxels in apical regions that were traversed by multiple fibres. We observed that both the mean generalised fractional anisotropy and mean kurtosis were lower in hearts in contracture compared to the slack state, by 23% and 9.3%, respectively. While its heavy acquisition burden currently limits the application of DSI in vivo, ongoing work in acceleration techniques may enable its use in live animals and patients. This would provide access to the as yet unexplored dimension of non-Gaussian diffusion that could serve as a highly sensitive marker of cardiac micro-structural integrity.
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Affiliation(s)
- Maelene Lohezic
- British Heart Foundation Experimental Magnetic Resonance Unit, Division of Cardiovascular Medicine, Radcliffe Department of Medicine, University of Oxford, Oxford, UK
| | - Irvin Teh
- British Heart Foundation Experimental Magnetic Resonance Unit, Division of Cardiovascular Medicine, Radcliffe Department of Medicine, University of Oxford, Oxford, UK
| | - Christian Bollensdorff
- National Heart and Lung Institute, Imperial College London, London, UK; Qatar Cardiovascular Research Center, Qatar Foundation, Doha, Qatar
| | - Rémi Peyronnet
- National Heart and Lung Institute, Imperial College London, London, UK
| | - Patrick W Hales
- Imaging and Biophysics Unit, Institute of Child Health, University College London, London, UK
| | - Vicente Grau
- Department of Engineering Science, University of Oxford, Oxford, UK
| | - Peter Kohl
- National Heart and Lung Institute, Imperial College London, London, UK; Department of Computer Science, University of Oxford, Oxford, UK
| | - Jürgen E Schneider
- British Heart Foundation Experimental Magnetic Resonance Unit, Division of Cardiovascular Medicine, Radcliffe Department of Medicine, University of Oxford, Oxford, UK.
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Abstract
Knowledge of cardiomyocyte biology is limited by the lack of methods to interrogate single-cell physiology in vivo. Here we show that contracting myocytes can indeed be imaged with optical microscopy at high temporal and spatial resolution in the beating murine heart, allowing visualization of individual sarcomeres and measurement of the single cardiomyocyte contractile cycle. Collectively, this has been enabled by efficient tissue stabilization, a prospective real-time cardiac gating approach, an image processing algorithm for motion-artifact-free imaging throughout the cardiac cycle, and a fluorescent membrane staining protocol. Quantification of cardiomyocyte contractile function in vivo opens many possibilities for investigating myocardial disease and therapeutic intervention at the cellular level.
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44
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Cardiac thin filament regulation and the Frank-Starling mechanism. J Physiol Sci 2014; 64:221-32. [PMID: 24788476 PMCID: PMC4070490 DOI: 10.1007/s12576-014-0314-y] [Citation(s) in RCA: 57] [Impact Index Per Article: 5.7] [Reference Citation Analysis] [Abstract] [Track Full Text] [Download PDF] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Received: 12/27/2013] [Accepted: 03/28/2014] [Indexed: 11/06/2022]
Abstract
The heart has an intrinsic ability to increase systolic force in response to a rise in ventricular filling (the Frank–Starling law of the heart). It is widely accepted that the length dependence of myocardial activation underlies the Frank–Starling law of the heart. Recent advances in muscle physiology have enabled the identification of the factors involved in length-dependent activation, viz., titin (connectin)-based interfilament lattice spacing reduction and thin filament “on–off” regulation, with the former triggering length-dependent activation and the latter determining the number of myosin molecules recruited to thin filaments. Patients with a failing heart have demonstrated reduced exercise tolerance at least in part via depression of the Frank–Starling mechanism. Recent studies revealed that various mutations occur in the thin filament regulatory proteins, such as troponin, in the ventricular muscle of failing hearts, which consequently alter the Frank–Starling mechanism. In this article, we review the molecular mechanisms of length-dependent activation, and the influence of troponin mutations on the phenomenon.
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45
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Garcia-Canadilla P, Gonzalez-Tendero A, Iruretagoyena I, Crispi F, Torre I, Amat-Roldan I, Bijnens BH, Gratacos E. Automated cardiac sarcomere analysis from second harmonic generation images. JOURNAL OF BIOMEDICAL OPTICS 2014; 19:056010. [PMID: 24853145 DOI: 10.1117/1.jbo.19.5.056010] [Citation(s) in RCA: 8] [Impact Index Per Article: 0.8] [Reference Citation Analysis] [Abstract] [MESH Headings] [Track Full Text] [Subscribe] [Scholar Register] [Received: 01/29/2014] [Accepted: 04/17/2014] [Indexed: 06/03/2023]
Abstract
Automatic quantification of cardiac muscle properties in tissue sections might provide important information related to different types of diseases. Second harmonic generation (SHG) imaging provides a stain-free microscopy approach to image cardiac fibers that, combined with our methodology of the automated measurement of the ultrastructure of muscle fibers, computes a reliable set of quantitative image features (sarcomere length, A-band length, thick-thin interaction length, and fiber orientation). We evaluated the performance of our methodology in computer-generated muscle fibers modeling some artifacts that are present during the image acquisition. Then, we also evaluated it by comparing it to manual measurements in SHG images from cardiac tissue of fetal and adult rabbits. The results showed a good performance of our methodology at high signal-to-noise ratio of 20 dB. We conclude that our automated measurements enable reliable characterization of cardiac fiber tissues to systematically study cardiac tissue in a wide range of conditions.
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Affiliation(s)
- Patricia Garcia-Canadilla
- University of Barcelona, BCNatal-Barcelona Center for Maternal-Fetal and Neonatal Medicine (Hospital Clínic and Hospital Sant Joan de Déu), IDIBAPS, and Centre for Biomedical Research on Rare Diseases (CIBER-ER), Barcelona 08028, SpainbUniversitat Pompeu
| | - Anna Gonzalez-Tendero
- University of Barcelona, BCNatal-Barcelona Center for Maternal-Fetal and Neonatal Medicine (Hospital Clínic and Hospital Sant Joan de Déu), IDIBAPS, and Centre for Biomedical Research on Rare Diseases (CIBER-ER), Barcelona 08028, Spain
| | - Igor Iruretagoyena
- University of Barcelona, BCNatal-Barcelona Center for Maternal-Fetal and Neonatal Medicine (Hospital Clínic and Hospital Sant Joan de Déu), IDIBAPS, and Centre for Biomedical Research on Rare Diseases (CIBER-ER), Barcelona 08028, Spain
| | - Fatima Crispi
- University of Barcelona, BCNatal-Barcelona Center for Maternal-Fetal and Neonatal Medicine (Hospital Clínic and Hospital Sant Joan de Déu), IDIBAPS, and Centre for Biomedical Research on Rare Diseases (CIBER-ER), Barcelona 08028, Spain
| | - Iratxe Torre
- University of Barcelona, BCNatal-Barcelona Center for Maternal-Fetal and Neonatal Medicine (Hospital Clínic and Hospital Sant Joan de Déu), IDIBAPS, and Centre for Biomedical Research on Rare Diseases (CIBER-ER), Barcelona 08028, Spain
| | - Ivan Amat-Roldan
- University of Barcelona, BCNatal-Barcelona Center for Maternal-Fetal and Neonatal Medicine (Hospital Clínic and Hospital Sant Joan de Déu), IDIBAPS, and Centre for Biomedical Research on Rare Diseases (CIBER-ER), Barcelona 08028, Spain
| | - Bart H Bijnens
- Universitat Pompeu Fabra, PhySense, DTIC, Barcelona 08018, SpaincICREA, Barcelona 08010, Spain
| | - Eduard Gratacos
- University of Barcelona, BCNatal-Barcelona Center for Maternal-Fetal and Neonatal Medicine (Hospital Clínic and Hospital Sant Joan de Déu), IDIBAPS, and Centre for Biomedical Research on Rare Diseases (CIBER-ER), Barcelona 08028, Spain
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Shintani SA, Oyama K, Kobirumaki-Shimozawa F, Ohki T, Ishiwata S, Fukuda N. Sarcomere length nanometry in rat neonatal cardiomyocytes expressed with α-actinin-AcGFP in Z discs. ACTA ACUST UNITED AC 2014; 143:513-24. [PMID: 24638993 PMCID: PMC3971663 DOI: 10.1085/jgp.201311118] [Citation(s) in RCA: 36] [Impact Index Per Article: 3.6] [Reference Citation Analysis] [Abstract] [Track Full Text] [Download PDF] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Indexed: 02/05/2023]
Abstract
Nanometry is widely used in biological sciences to analyze the movement of molecules or molecular assemblies in cells and in vivo. In cardiac muscle, a change in sarcomere length (SL) by a mere ∼100 nm causes a substantial change in contractility, indicating the need for the simultaneous measurement of SL and intracellular Ca(2+) concentration ([Ca(2+)]i) in cardiomyocytes at high spatial and temporal resolution. To accurately analyze the motion of individual sarcomeres with nanometer precision during excitation-contraction coupling, we applied nanometry techniques to primary-cultured rat neonatal cardiomyocytes. First, we developed an experimental system for simultaneous nanoscale analysis of single sarcomere dynamics and [Ca(2+)]i changes via the expression of AcGFP in Z discs. We found that the averaging of the lengths of sarcomeres along the myocyte, a method generally used in today's myocardial research, caused marked underestimation of sarcomere lengthening speed because of the superpositioning of different timings for lengthening between sequentially connected sarcomeres. Then, we found that after treatment with ionomycin, neonatal myocytes exhibited spontaneous sarcomeric oscillations (cell-SPOCs) at partial activation with blockage of sarcoplasmic reticulum functions, and the waveform properties were indistinguishable from those obtained in electric field stimulation. The myosin activator omecamtiv mecarbil markedly enhanced Z-disc displacement during cell-SPOC. Finally, we interpreted the present experimental findings in the framework of our mathematical model of SPOCs. The present experimental system has a broad range of application possibilities for unveiling single sarcomere dynamics during excitation-contraction coupling in cardiomyocytes under various settings.
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Affiliation(s)
- Seine A Shintani
- Department of Pure and Applied Physics, Faculty of Science and Engineering, Waseda University, Shinjuku-ku, Tokyo 169-8555, Japan
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47
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Botcherby EJ, Corbett A, Burton RAB, Smith CW, Bollensdorff C, Booth MJ, Kohl P, Wilson T, Bub G. Fast measurement of sarcomere length and cell orientation in Langendorff-perfused hearts using remote focusing microscopy. Circ Res 2013; 113:863-70. [PMID: 23899961 DOI: 10.1161/circresaha.113.301704] [Citation(s) in RCA: 27] [Impact Index Per Article: 2.5] [Reference Citation Analysis] [Abstract] [Key Words] [Track Full Text] [Journal Information] [Submit a Manuscript] [Subscribe] [Scholar Register] [Indexed: 11/16/2022]
Abstract
RATIONALE Sarcomere length (SL) is a key indicator of cardiac mechanical function, but current imaging technologies are limited in their ability to unambiguously measure and characterize SL at the cell level in intact, living tissue. OBJECTIVE We developed a method for measuring SL and regional cell orientation using remote focusing microscopy, an emerging imaging modality that can capture light from arbitrary oblique planes within a sample. METHODS AND RESULTS We present a protocol that unambiguously and quickly determines cell orientation from user-selected areas in a field of view by imaging 2 oblique planes that share a common major axis with the cell. We demonstrate the effectiveness of the technique in establishing single-cell SL in Langendorff-perfused hearts loaded with the membrane dye di-4-ANEPPS. CONCLUSIONS Remote focusing microscopy can measure cell orientation in complex 2-photon data sets without capturing full z stacks. The technique allows rapid assessment of SL in healthy and diseased heart experimental preparations.
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48
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Peterson P, Kalda M, Vendelin M. Real-time determination of sarcomere length of a single cardiomyocyte during contraction. Am J Physiol Cell Physiol 2012; 304:C519-31. [PMID: 23255581 PMCID: PMC3671565 DOI: 10.1152/ajpcell.00032.2012] [Citation(s) in RCA: 20] [Impact Index Per Article: 1.7] [Reference Citation Analysis] [Abstract] [Track Full Text] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Indexed: 11/22/2022]
Abstract
Sarcomere length of a cardiomyocyte is an important control parameter for physiology studies on a single cell level; for instance, its accurate determination in real time is essential for performing single cardiomyocyte contraction experiments. The aim of this work is to develop an efficient and accurate method for estimating a mean sarcomere length of a contracting cardiomyocyte using microscopy images as an input. The novelty in developed method lies in 1) using unbiased measure of similarities to eliminate systematic errors from conventional autocorrelation function (ACF)-based methods when applied to region of interest of an image, 2) using a semianalytical, seminumerical approach for evaluating the similarity measure to take into account spatial dependence of neighboring image pixels, and 3) using a detrend algorithm to extract the sarcomere striation pattern content from the microscopy images. The developed sarcomere length estimation procedure has superior computational efficiency and estimation accuracy compared with the conventional ACF and spectral analysis-based methods using fast Fourier transform. As shown by analyzing synthetic images with the known periodicity, the estimates obtained by the developed method are more accurate at the subpixel level than ones obtained using ACF analysis. When applied in practice on rat cardiomyocytes, our method was found to be robust to the choice of the region of interest that may 1) include projections of carbon fibers and nucleus, 2) have uneven background, and 3) be slightly disoriented with respect to average direction of sarcomere striation pattern. The developed method is implemented in open-source software.
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Affiliation(s)
- Pearu Peterson
- Laboratory of Systems Biology, Institute of Cybernetics, Tallinn University of Technology, Akadeemia 21, 12618 Tallinn, Estonia.
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49
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Pett K, Hauton D. The effects of asymmetric ventricular filling on left-right ventricular interaction in the normal rat heart. Pflugers Arch 2012; 464:523-34. [PMID: 23001120 DOI: 10.1007/s00424-012-1154-3] [Citation(s) in RCA: 0] [Impact Index Per Article: 0] [Reference Citation Analysis] [Abstract] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Received: 08/09/2012] [Revised: 08/31/2012] [Accepted: 09/04/2012] [Indexed: 11/28/2022]
Abstract
Heart failure is characterised by ventricular dysfunction and with the potential for changes to ventricular volumes constraining the mechanical performance of the heart. The contribution of this interaction from geometric changes rather than fibrosis or metabolic changes is unclear. Using the constant pressure Langendorff-perfused rat heart, the volume interaction between left ventricle (LV) and right ventricle (RV) was investigated. RV diastolic stiffness (P < 0.001) and developed pressure (P < 0.001) were significantly lower than LV. When the RV was fixed at the end-diastolic volume (EDV) or EDV + 50 %, both LV systolic and diastolic performance were unaffected with increasing LV balloon volume. However, at fixed LV volume, RV systolic performance was significantly decreased when LV volume increased to EDV + 50 % when RV volume was increased incrementally between 50 and 300 μl (P < 0.001). Systolic interaction in RV was noted as declining RV peak systolic load with increasing LV systolic pressure (P < 0.05) and diastolic interaction was noted for RV when LV volume was increased from EDV to EDV + 50 % (P < 0.05). RV diastolic wall stress was increased with increasing LV balloon volume (P < 0.05), but LV wall stress was unaltered at fixed RV balloon volume. Taken together, increasing LV volume above EDV decreased systolic performance and triggered ventricular constraint in the RV but the RV itself had no effect on the performance of the LV. These results are consistent with overload of the LV impairing pulmonary perfusion by direct ventricular interaction with potential alteration to ventilation-perfusion characteristics within the lung.
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Affiliation(s)
- Kimberley Pett
- School of Clinical and Experimental Medicine, College of Medical and Dental Sciences, University of Birmingham, Edgbaston, Birmingham, B15 2TT, UK
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Histo-anatomical structure of the living isolated rat heart in two contraction states assessed by diffusion tensor MRI. PROGRESS IN BIOPHYSICS AND MOLECULAR BIOLOGY 2012; 110:319-30. [PMID: 23043978 PMCID: PMC3526796 DOI: 10.1016/j.pbiomolbio.2012.07.014] [Citation(s) in RCA: 95] [Impact Index Per Article: 7.9] [Reference Citation Analysis] [Abstract] [Track Full Text] [Figures] [Subscribe] [Scholar Register] [Received: 07/26/2012] [Accepted: 07/30/2012] [Indexed: 11/21/2022]
Abstract
Deformation and wall-thickening of ventricular myocardium are essential for cardiac pump function. However, insight into the histo-anatomical basis for cardiac tissue re-arrangement during contraction is limited. In this report, we describe dynamic changes in regionally prevailing cardiomyocyte (fibre) and myolaminar (sheet) orientations, using Diffusion Tensor Imaging (DTI) of ventricles in the same living heart in two different mechanical states. Hearts, isolated from Sprague–Dawley rats, were Langendorff-perfused and imaged, initially in their slack state during cardioplegic arrest, then during lithium-induced contracture. Regional fibre- and sheet-orientations were derived from DTI-data on a voxel-wise basis. Contraction was accompanied with a decrease in left-handed helical fibres (handedness relative to the baso-apical direction) in basal, equatorial, and apical sub-epicardium (by 14.0%, 17.3%, 15.8% respectively; p < 0.001), and an increase in right-handed helical fibres of the sub-endocardium (by 11.0%, 12.1% and 16.1%, respectively; p < 0.001). Two predominant sheet-populations were observed, with sheet-angles of either positive (β+) or negative (β−) polarity relative to a ‘chamber-horizontal plane’ (defined as normal to the left ventricular long-axis). In contracture, mean ‘intersection’-angle (geometrically quantifiable intersection of sheet-angle projections) between β+ and β− sheet-populations increased from 86.2 ± 5.5° (slack) to 108.3 ± 5.4° (p < 0.001). Subsequent high-resolution DTI of fixed myocardium, and histological sectioning, reconfirmed the existence of alternating sheet-plane populations. Our results suggest that myocardial tissue layers in alternating sheet-populations align into a more chamber-horizontal orientation during contraction. This re-arrangement occurs via an accordion-like mechanism that, combined with inter-sheet slippage, can significantly contribute to ventricular deformation, including wall-thickening in a predominantly centripetal direction and baso-apical shortening.
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