1
|
Wenqiang D, Novin A, Liu Y, Afzal J, Suhail Y, Liu S, Gavin NR, Jorgensen JR, Morosky CM, Figueroa R, Schmidt TA, Sanders M, Brewer MA, Kshitiz. Scar matrix drives Piezo1 mediated stromal inflammation leading to placenta accreta spectrum. Nat Commun 2024; 15:8379. [PMID: 39333481 DOI: 10.1038/s41467-024-52351-0] [Citation(s) in RCA: 0] [Impact Index Per Article: 0] [Reference Citation Analysis] [Abstract] [MESH Headings] [Grants] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Received: 01/31/2023] [Accepted: 09/03/2024] [Indexed: 09/29/2024] Open
Abstract
Scar tissue formation is a hallmark of wound repair in adults and can chronically affect tissue architecture and function. To understand the general phenomena, we sought to explore scar-driven imbalance in tissue homeostasis caused by a common, and standardized surgical procedure, the uterine scar due to cesarean surgery. Deep uterine scar is associated with a rapidly increasing condition in pregnant women, placenta accreta spectrum (PAS), characterized by aggressive trophoblast invasion into the uterus, frequently necessitating hysterectomy at parturition. We created a model of uterine scar, recapitulating PAS-like invasive phenotype, showing that scar matrix activates mechanosensitive ion channel, Piezo1, through glycolysis-fueled cellular contraction. Piezo1 activation increases intracellular calcium activity and Protein kinase C activation, leading to NF-κB nuclear translocation, and MafG stabilization. This inflammatory transformation of decidua leads to production of IL-8 and G-CSF, chemotactically recruiting invading trophoblasts towards scar, initiating PAS. Our study demonstrates aberrant mechanics of scar disturbs stroma-epithelia homeostasis in placentation, with implications in cancer dissemination.
Collapse
Affiliation(s)
- Du Wenqiang
- Department of Biomedical Engineering, University of Connecticut Health Center, Farmington, CT, USA
- Department of Biomedical Engineering, University of Connecticut, Storrs, CT, USA
| | - Ashkan Novin
- Department of Biomedical Engineering, University of Connecticut Health Center, Farmington, CT, USA
- Department of Biomedical Engineering, University of Connecticut, Storrs, CT, USA
| | - Yamin Liu
- Department of Biomedical Engineering, University of Connecticut, Storrs, CT, USA
| | - Junaid Afzal
- Division of Cardiology, Department of Medicine, University of California San Francisco, San Francisco, CA, USA
| | - Yasir Suhail
- Department of Biomedical Engineering, University of Connecticut Health Center, Farmington, CT, USA
- Department of Biomedical Engineering, University of Connecticut, Storrs, CT, USA
| | - Shaofei Liu
- Department of Biomedical Engineering, University of Connecticut Health Center, Farmington, CT, USA
- Department of Biomedical Engineering, University of Connecticut, Storrs, CT, USA
| | - Nicole R Gavin
- Department of Obstetrics and Gynecology, University of Connecticut Health Center, Farmington, CT, USA
| | - Jennifer R Jorgensen
- Department of Obstetrics and Gynecology, University of Connecticut Health Center, Farmington, CT, USA
| | - Christopher M Morosky
- Department of Obstetrics and Gynecology, University of Connecticut Health Center, Farmington, CT, USA
| | - Reinaldo Figueroa
- Department of Obstetrics and Gynecology, Saint Francis Hospital and Medical Center, Hartford, CT, USA
| | - Tannin A Schmidt
- Department of Biomedical Engineering, University of Connecticut Health Center, Farmington, CT, USA
| | - Melinda Sanders
- Department of Obstetrics and Gynecology, University of Connecticut Health Center, Farmington, CT, USA
- Department of Pathology, University of Connecticut Health Center, Farmington, CT, USA
| | - Molly A Brewer
- Department of Obstetrics and Gynecology, University of Connecticut Health Center, Farmington, CT, USA
| | - Kshitiz
- Department of Biomedical Engineering, University of Connecticut Health Center, Farmington, CT, USA.
- Department of Biomedical Engineering, University of Connecticut, Storrs, CT, USA.
| |
Collapse
|
2
|
Jin XK, Jin KQ, Yang XK, Wen MY, Liu YL, Huang WH. Real-time monitoring of intracellular biochemical response in locally stretched single cell by a nanosensor. Anal Bioanal Chem 2024; 416:4779-4787. [PMID: 38802680 DOI: 10.1007/s00216-024-05348-z] [Citation(s) in RCA: 0] [Impact Index Per Article: 0] [Reference Citation Analysis] [Abstract] [Key Words] [MESH Headings] [Grants] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Received: 03/10/2024] [Revised: 04/27/2024] [Accepted: 05/17/2024] [Indexed: 05/29/2024]
Abstract
Mechanotransduction is the essential process that cells convert mechanical force into biochemical responses, and electrochemical sensor stands out from existing techniques by providing quantitative and real-time information about the biochemical signals during cellular mechanotransduction. However, the intracellular biochemical response evoked by mechanical force has been poorly monitored. In this paper, we report a method to apply local stretch on single cell and simultaneously monitor the ensuing intracellular biochemical signals. Specifically, a ferromagnetic micropipette was fabricated to locally stretch a single cell labeled with Fe3O4 nanoparticles under the external magnetic field, and the SiC@Pt nanowire electrode (SiC@Pt NWE) was inserted into the cell to monitor the intracellular hydrogen peroxide (H2O2) production induced by the local stretch. As a proof of concept, this work quantitatively investigated the elevated amount of H2O2 levels in single endothelial cell under different stretching amplitudes. This work puts forward a new research modality to manipulate and monitor the mechanotransduction at the single-cell level.
Collapse
Affiliation(s)
- Xue-Ke Jin
- College of Chemistry and Molecular Sciences, Wuhan University, Wuhan, 430072, China
| | - Kai-Qi Jin
- College of Chemistry and Molecular Sciences, Wuhan University, Wuhan, 430072, China
| | - Xiao-Ke Yang
- College of Chemistry and Molecular Sciences, Wuhan University, Wuhan, 430072, China
| | - Ming-Yong Wen
- College of Chemistry and Molecular Sciences, Wuhan University, Wuhan, 430072, China
| | - Yan-Ling Liu
- College of Chemistry and Molecular Sciences, Wuhan University, Wuhan, 430072, China
| | - Wei-Hua Huang
- College of Chemistry and Molecular Sciences, Wuhan University, Wuhan, 430072, China.
| |
Collapse
|
3
|
Rogers J, Bajur AT, Salaita K, Spillane KM. Mechanical control of antigen detection and discrimination by T and B cell receptors. Biophys J 2024; 123:2234-2255. [PMID: 38794795 PMCID: PMC11331051 DOI: 10.1016/j.bpj.2024.05.020] [Citation(s) in RCA: 0] [Impact Index Per Article: 0] [Reference Citation Analysis] [Abstract] [MESH Headings] [Grants] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Received: 02/14/2024] [Revised: 05/10/2024] [Accepted: 05/21/2024] [Indexed: 05/26/2024] Open
Abstract
The adaptive immune response is orchestrated by just two cell types, T cells and B cells. Both cells possess the remarkable ability to recognize virtually any antigen through their respective antigen receptors-the T cell receptor (TCR) and B cell receptor (BCR). Despite extensive investigations into the biochemical signaling events triggered by antigen recognition in these cells, our ability to predict or control the outcome of T and B cell activation remains elusive. This challenge is compounded by the sensitivity of T and B cells to the biophysical properties of antigens and the cells presenting them-a phenomenon we are just beginning to understand. Recent insights underscore the central role of mechanical forces in this process, governing the conformation, signaling activity, and spatial organization of TCRs and BCRs within the cell membrane, ultimately eliciting distinct cellular responses. Traditionally, T cells and B cells have been studied independently, with researchers working in parallel to decipher the mechanisms of activation. While these investigations have unveiled many overlaps in how these cell types sense and respond to antigens, notable differences exist. To fully grasp their biology and harness it for therapeutic purposes, these distinctions must be considered. This review compares and contrasts the TCR and BCR, placing emphasis on the role of mechanical force in regulating the activity of both receptors to shape cellular and humoral adaptive immune responses.
Collapse
Affiliation(s)
- Jhordan Rogers
- Department of Chemistry, Emory University, Atlanta, Georgia
| | - Anna T Bajur
- Department of Physics, King's College London, London, United Kingdom; Randall Centre for Cell and Molecular Biophysics, King's College London, London, United Kingdom
| | - Khalid Salaita
- Department of Chemistry, Emory University, Atlanta, Georgia; Wallace H. Coulter Department of Biomedical Engineering, Georgia Institute of Technology and Emory University, Atlanta, Georgia.
| | - Katelyn M Spillane
- Department of Physics, King's College London, London, United Kingdom; Randall Centre for Cell and Molecular Biophysics, King's College London, London, United Kingdom; Department of Life Sciences, Imperial College London, London, United Kingdom.
| |
Collapse
|
4
|
Kołodziej T, Mrózek M, Sengottuvel S, Głowacki MJ, Ficek M, Gawlik W, Rajfur Z, Wojciechowski AM. Multimodal analysis of traction forces and the temperature dynamics of living cells with a diamond-embedded substrate. BIOMEDICAL OPTICS EXPRESS 2024; 15:4024-4043. [PMID: 39022544 PMCID: PMC11249686 DOI: 10.1364/boe.524293] [Citation(s) in RCA: 0] [Impact Index Per Article: 0] [Reference Citation Analysis] [Abstract] [Track Full Text] [Figures] [Subscribe] [Scholar Register] [Received: 03/19/2024] [Revised: 04/30/2024] [Accepted: 04/30/2024] [Indexed: 07/20/2024]
Abstract
Cells and tissues are constantly exposed to chemical and physical signals that regulate physiological and pathological processes. This study explores the integration of two biophysical methods: traction force microscopy (TFM) and optically detected magnetic resonance (ODMR) to concurrently assess cellular traction forces and the local relative temperature. We present a novel elastic substrate with embedded nitrogen-vacancy microdiamonds that facilitate ODMR-TFM measurements. Optimization efforts focused on minimizing sample illumination and experiment duration to mitigate biological perturbations. Our hybrid ODMR-TFM technique yields TFM maps and achieves approximately 1 K precision in relative temperature measurements. Our setup employs a simple wide-field fluorescence microscope with standard components, demonstrating the feasibility of the proposed technique in life science laboratories. By elucidating the physical aspects of cellular behavior beyond the existing methods, this approach opens avenues for a deeper understanding of cellular processes and may inspire the development of diverse biomedical applications.
Collapse
Affiliation(s)
- Tomasz Kołodziej
- Jagiellonian University Medical School, Faculty of Pharmacy, Kraków, Poland
- Jagiellonian University , Faculty of Physics, Astronomy, and Applied Computer Science, Kraków, Poland
| | - Mariusz Mrózek
- Jagiellonian University , Faculty of Physics, Astronomy, and Applied Computer Science, Kraków, Poland
| | - Saravanan Sengottuvel
- Jagiellonian University , Faculty of Physics, Astronomy, and Applied Computer Science, Kraków, Poland
- Jagiellonian University, Doctoral School of Exact and Natural Sciences, Kraków, Poland
| | - Maciej J Głowacki
- Gdansk University of Technology, Faculty of Electronics, Telecommunications, and Informatics, Department of Metrology and Optoelectronics, Gdańsk, Poland
| | - Mateusz Ficek
- Gdansk University of Technology, Faculty of Electronics, Telecommunications, and Informatics, Department of Metrology and Optoelectronics, Gdańsk, Poland
| | - Wojciech Gawlik
- Jagiellonian University , Faculty of Physics, Astronomy, and Applied Computer Science, Kraków, Poland
| | - Zenon Rajfur
- Jagiellonian University , Faculty of Physics, Astronomy, and Applied Computer Science, Kraków, Poland
| | - Adam M Wojciechowski
- Jagiellonian University , Faculty of Physics, Astronomy, and Applied Computer Science, Kraków, Poland
| |
Collapse
|
5
|
Chen H, Wang S, Cao Y, Lei H. Molecular Force Sensors for Biological Application. Int J Mol Sci 2024; 25:6198. [PMID: 38892386 PMCID: PMC11173168 DOI: 10.3390/ijms25116198] [Citation(s) in RCA: 0] [Impact Index Per Article: 0] [Reference Citation Analysis] [Abstract] [Key Words] [MESH Headings] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Received: 04/29/2024] [Revised: 05/29/2024] [Accepted: 05/29/2024] [Indexed: 06/21/2024] Open
Abstract
The mechanical forces exerted by cells on their surrounding microenvironment are known as cellular traction forces. These forces play crucial roles in various biological processes, such as tissue development, wound healing and cell functions. However, it is hard for traditional techniques to measure cellular traction forces accurately because their magnitude (from pN to nN) and the length scales over which they occur (from nm to μm) are extremely small. In order to fully understand mechanotransduction, highly sensitive tools for measuring cellular forces are needed. Current powerful techniques for measuring traction forces include traction force microscopy (TFM) and fluorescent molecular force sensors (FMFS). In this review, we elucidate the force imaging principles of TFM and FMFS. Then we highlight the application of FMFS in a variety of biological processes and offer our perspectives and insights into the potential applications of FMFS.
Collapse
Affiliation(s)
- Huiyan Chen
- National Laboratory of Solid State Microstructure, Department of Physics, Nanjing University, Nanjing 210093, China; (H.C.); (S.W.)
| | - Shouhan Wang
- National Laboratory of Solid State Microstructure, Department of Physics, Nanjing University, Nanjing 210093, China; (H.C.); (S.W.)
| | - Yi Cao
- National Laboratory of Solid State Microstructure, Department of Physics, Nanjing University, Nanjing 210093, China; (H.C.); (S.W.)
| | - Hai Lei
- School of Physics, Zhejiang University, Hangzhou 310027, China
- Institute for Advanced Study in Physics, Zhejiang University, Hangzhou 310027, China
| |
Collapse
|
6
|
Karimi A, Aga M, Khan T, D'costa SD, Thaware O, White E, Kelley MJ, Gong H, Acott TS. Comparative analysis of traction forces in normal and glaucomatous trabecular meshwork cells within a 3D, active fluid-structure interaction culture environment. Acta Biomater 2024; 180:206-229. [PMID: 38641184 PMCID: PMC11095374 DOI: 10.1016/j.actbio.2024.04.021] [Citation(s) in RCA: 0] [Impact Index Per Article: 0] [Reference Citation Analysis] [Abstract] [Key Words] [MESH Headings] [Grants] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Received: 12/20/2023] [Revised: 03/26/2024] [Accepted: 04/11/2024] [Indexed: 04/21/2024]
Abstract
This study presents a 3D in vitro cell culture model, meticulously 3D printed to replicate the conventional aqueous outflow pathway anatomical structure, facilitating the study of trabecular meshwork (TM) cellular responses under glaucomatous conditions. Glaucoma affects TM cell functionality, leading to extracellular matrix (ECM) stiffening, enhanced cell-ECM adhesion, and obstructed aqueous humor outflow. Our model, reconstructed from polyacrylamide gel with elastic moduli of 1.5 and 21.7 kPa, is based on serial block-face scanning electron microscopy images of the outflow pathway. It allows for quantifying 3D, depth-dependent, dynamic traction forces exerted by both normal and glaucomatous TM cells within an active fluid-structure interaction (FSI) environment. In our experimental design, we designed two scenarios: a control group with TM cells observed over 20 hours without flow (static setting), focusing on intrinsic cellular contractile forces, and a second scenario incorporating active FSI to evaluate its impact on traction forces (dynamic setting). Our observations revealed that active FSI results in higher traction forces (normal: 1.83-fold and glaucoma: 2.24-fold) and shear strains (normal: 1.81-fold and glaucoma: 2.41-fold), with stiffer substrates amplifying this effect. Glaucomatous cells consistently exhibited larger forces than normal cells. Increasing gel stiffness led to enhanced stress fiber formation in TM cells, particularly in glaucomatous cells. Exposure to active FSI dramatically altered actin organization in both normal and glaucomatous TM cells, particularly affecting cortical actin stress fiber arrangement. This model while preliminary offers a new method in understanding TM cell biomechanics and ECM stiffening in glaucoma, highlighting the importance of FSI in these processes. STATEMENT OF SIGNIFICANCE: This pioneering project presents an advanced 3D in vitro model, meticulously replicating the human trabecular meshwork's anatomy for glaucoma research. It enables precise quantification of cellular forces in a dynamic fluid-structure interaction, a leap forward from existing 2D models. This advancement promises significant insights into trabecular meshwork cell biomechanics and the stiffening of the extracellular matrix in glaucoma, offering potential pathways for innovative treatments. This research is positioned at the forefront of ocular disease study, with implications that extend to broader biomedical applications.
Collapse
Affiliation(s)
- Alireza Karimi
- Department of Ophthalmology, Casey Eye Institute, Oregon Health & Science University, Portland, OR, United States; Department of Biomedical Engineering, Oregon Health & Science University, Portland, OR, United States.
| | - Mini Aga
- Department of Ophthalmology, Casey Eye Institute, Oregon Health & Science University, Portland, OR, United States
| | - Taaha Khan
- Department of Ophthalmology, Casey Eye Institute, Oregon Health & Science University, Portland, OR, United States
| | - Siddharth Daniel D'costa
- Department of Ophthalmology, Casey Eye Institute, Oregon Health & Science University, Portland, OR, United States
| | - Omkar Thaware
- Department of Ophthalmology, Casey Eye Institute, Oregon Health & Science University, Portland, OR, United States; Department of Biomedical Engineering, Oregon Health & Science University, Portland, OR, United States
| | - Elizabeth White
- Department of Ophthalmology, Casey Eye Institute, Oregon Health & Science University, Portland, OR, United States
| | - Mary J Kelley
- Department of Ophthalmology, Casey Eye Institute, Oregon Health & Science University, Portland, OR, United States; Department Integrative Biosciences, School of Dentistry, Oregon Health & Science University, Portland, OR, United States
| | - Haiyan Gong
- Department of Ophthalmology, Boston University School of Medicine, Boston, MA, United States; Department of Anatomy and Neurobiology, Boston University School of Medicine, Boston, MA, United States
| | - Ted S Acott
- Department of Ophthalmology, Casey Eye Institute, Oregon Health & Science University, Portland, OR, United States; Department Chemical Physiology & Biochemistry, School of Medicine, Oregon Health & Science University, Portland, OR, United States
| |
Collapse
|
7
|
Denisin AK, Kim H, Riedel-Kruse IH, Pruitt BL. Field Guide to Traction Force Microscopy. Cell Mol Bioeng 2024; 17:87-106. [PMID: 38737454 PMCID: PMC11082129 DOI: 10.1007/s12195-024-00801-6] [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: 01/01/2024] [Accepted: 03/26/2024] [Indexed: 05/14/2024] Open
Abstract
Introduction Traction force microscopy (TFM) is a widely used technique to measure cell contractility on compliant substrates that mimic the stiffness of human tissues. For every step in a TFM workflow, users make choices which impact the quantitative results, yet many times the rationales and consequences for making these decisions are unclear. We have found few papers which show the complete experimental and mathematical steps of TFM, thus obfuscating the full effects of these decisions on the final output. Methods Therefore, we present this "Field Guide" with the goal to explain the mathematical basis of common TFM methods to practitioners in an accessible way. We specifically focus on how errors propagate in TFM workflows given specific experimental design and analytical choices. Results We cover important assumptions and considerations in TFM substrate manufacturing, substrate mechanical properties, imaging techniques, image processing methods, approaches and parameters used in calculating traction stress, and data-reporting strategies. Conclusions By presenting a conceptual review and analysis of TFM-focused research articles published over the last two decades, we provide researchers in the field with a better understanding of their options to make more informed choices when creating TFM workflows depending on the type of cell being studied. With this review, we aim to empower experimentalists to quantify cell contractility with confidence. Supplementary Information The online version contains supplementary material available at 10.1007/s12195-024-00801-6.
Collapse
Affiliation(s)
| | - Honesty Kim
- Department of Bioengineering, Stanford University, Stanford, CA 94305 USA
- Present Address: The Department of Pharmaceutical Chemistry, University of California, San Francisco, CA 94158 USA
- Department of Molecular and Cellular Biology, and (by courtesy) Departments of Biomedical Engineering, Applied Mathematics, and Physics, University of Arizona, Tucson, AZ 85721 USA
| | - Ingmar H. Riedel-Kruse
- Department of Molecular and Cellular Biology, and (by courtesy) Departments of Biomedical Engineering, Applied Mathematics, and Physics, University of Arizona, Tucson, AZ 85721 USA
| | - Beth L. Pruitt
- Departments of Bioengineering and Mechanical Engineering, University of California Santa Barbara, Santa Barbara, CA 93106 USA
| |
Collapse
|
8
|
Karimi A, Aga M, Khan T, D'costa SD, Cardenas-Riumallo S, Zelenitz M, Kelley MJ, Acott TS. Dynamic traction force in trabecular meshwork cells: A 2D culture model for normal and glaucomatous states. Acta Biomater 2024; 175:138-156. [PMID: 38151067 PMCID: PMC10843681 DOI: 10.1016/j.actbio.2023.12.033] [Citation(s) in RCA: 0] [Impact Index Per Article: 0] [Reference Citation Analysis] [Abstract] [Key Words] [MESH Headings] [Grants] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Received: 10/10/2023] [Revised: 12/10/2023] [Accepted: 12/20/2023] [Indexed: 12/29/2023]
Abstract
Glaucoma, which is associated with intraocular pressure (IOP) elevation, results in trabecular meshwork (TM) cellular dysfunction, leading to increased rigidity of the extracellular matrix (ECM), larger adhesion forces between the TM cells and ECM, and higher resistance to aqueous humor drainage. TM cells sense the mechanical forces due to IOP dynamic and apply multidimensional forces on the ECM. Recognizing the importance of cellular forces in modulating various cellular activities and development, this study is aimed to develop a 2D in vitro cell culture model to calculate the 3D, depth-dependent, dynamic traction forces, tensile/compressive/shear strain of the normal and glaucomatous human TM cells within a deformable polyacrylamide (PAM) gel substrate. Normal and glaucomatous human TM cells were isolated, cultured, and seeded on top of the PAM gel substrate with embedded FluoSpheres, spanning elastic moduli of 1.5 to 80 kPa. Sixteen-hour post-seeding live confocal microscopy in an incubator was conducted to Z-stack image the 3D displacement map of the FluoSpheres within the PAM gels. Combined with the known PAM gel stiffness, we ascertained the 3D traction forces in the gel. Our results revealed meaningfully larger traction forces in the glaucomatous TM cells compared to the normal TM cells, reaching depths greater than 10-µm in the PAM gel substrate. Stress fibers in TM cells increased with gel rigidity, but diminished when stiffness rose from 20 to 80 kPa. The developed 2D cell culture model aids in understanding how altered mechanical properties in glaucoma impact TM cell behavior and aqueous humor outflow resistance. STATEMENT OF SIGNIFICANCE: Glaucoma, a leading cause of irreversible blindness, is intricately linked to elevated intraocular pressures and their subsequent cellular effects. The trabecular meshwork plays a pivotal role in this mechanism, particularly its interaction with the extracellular matrix. This research unveils an advanced 2D in vitro cell culture model that intricately maps the complex 3D forces exerted by trabecular meshwork cells on the extracellular matrix, offering unparalleled insights into the cellular biomechanics at play in both healthy and glaucomatous eyes. By discerning the changes in these forces across varying substrate stiffness levels, we bridge the gap in understanding between cellular mechanobiology and the onset of glaucoma. The findings stand as a beacon for potential therapeutic avenues, emphasizing the gravity of cellular/extracellular matrix interactions in glaucoma's pathogenesis and setting the stage for targeted interventions in its early stages.
Collapse
Affiliation(s)
- Alireza Karimi
- Department of Ophthalmology, Casey Eye Institute, Oregon Health & Science University, Portland, OR, USA; Department of Biomedical Engineering, Oregon Health & Science University, Portland, OR, USA.
| | - Mini Aga
- Department of Ophthalmology, Casey Eye Institute, Oregon Health & Science University, Portland, OR, USA
| | - Taaha Khan
- Department of Ophthalmology, Casey Eye Institute, Oregon Health & Science University, Portland, OR, USA
| | - Siddharth Daniel D'costa
- Department of Ophthalmology, Casey Eye Institute, Oregon Health & Science University, Portland, OR, USA
| | | | - Meadow Zelenitz
- Department of Ophthalmology, Casey Eye Institute, Oregon Health & Science University, Portland, OR, USA
| | - Mary J Kelley
- Department of Ophthalmology, Casey Eye Institute, Oregon Health & Science University, Portland, OR, USA; Department Integrative Biosciences, School of Dentistry, Oregon Health & Science University, Portland, OR, USA
| | - Ted S Acott
- Department of Ophthalmology, Casey Eye Institute, Oregon Health & Science University, Portland, OR, USA; Department Chemical Physiology & Biochemistry, School of Medicine, Oregon Health & Science University, Portland, OR, USA
| |
Collapse
|
9
|
Wang W, Chen W, Wu C, Zhang C, Feng J, Liu P, Hu Y, Li H, Sun F, Jiang K, Zhang X, Liu Z. Hydrogel-based molecular tension fluorescence microscopy for investigating receptor-mediated rigidity sensing. Nat Methods 2023; 20:1780-1789. [PMID: 37798478 DOI: 10.1038/s41592-023-02037-0] [Citation(s) in RCA: 1] [Impact Index Per Article: 1.0] [Reference Citation Analysis] [Abstract] [MESH Headings] [Grants] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Received: 10/31/2022] [Accepted: 09/05/2023] [Indexed: 10/07/2023]
Abstract
Extracellular matrix (ECM) rigidity serves as a crucial mechanical cue impacting diverse biological processes. However, understanding the molecular mechanisms of rigidity sensing has been limited by the spatial resolution and force sensitivity of current cellular force measurement techniques. Here we developed a method to functionalize DNA tension probes on soft hydrogel surfaces in a controllable and reliable manner, enabling molecular tension fluorescence microscopy for rigidity sensing studies. Our findings showed that fibroblasts respond to substrate rigidity by recruiting more force-bearing integrins and modulating integrin sampling frequency of the ECM, rather than simply overloading the existing integrin-ligand bonds, to promote focal adhesion maturation. We also demonstrated that ECM rigidity positively regulates the pN force of T cell receptor-ligand bond and T cell receptor mechanical sampling frequency, promoting T cell activation. Thus, hydrogel-based molecular tension fluorescence microscopy implemented on a standard confocal microscope provides a simple and effective means to explore detailed molecular force information for rigidity-dependent biological processes.
Collapse
Affiliation(s)
- Wenxu Wang
- TaiKang Center for Life and Medical Sciences, the Institute for Advanced Studies, Wuhan University, Wuhan, China
| | - Wei Chen
- TaiKang Center for Life and Medical Sciences, the Institute for Advanced Studies, Wuhan University, Wuhan, China
| | - Chaoyang Wu
- TaiKang Center for Life and Medical Sciences, the Institute for Advanced Studies, Wuhan University, Wuhan, China
| | - Chen Zhang
- College of Life Sciences, Wuhan University, Wuhan, China
| | - Jingjing Feng
- TaiKang Center for Life and Medical Sciences, the Institute for Advanced Studies, Wuhan University, Wuhan, China
| | - Pengxiang Liu
- TaiKang Center for Life and Medical Sciences, the Institute for Advanced Studies, Wuhan University, Wuhan, China
| | - Yuru Hu
- TaiKang Center for Life and Medical Sciences, the Institute for Advanced Studies, Wuhan University, Wuhan, China
| | - Hongyun Li
- TaiKang Center for Life and Medical Sciences, the Institute for Advanced Studies, Wuhan University, Wuhan, China
| | - Feng Sun
- TaiKang Center for Life and Medical Sciences, the Institute for Advanced Studies, Wuhan University, Wuhan, China
| | - Kai Jiang
- Frontier Science Center for Immunology and Metabolism, Medical Research Institute, Wuhan University, Wuhan, China
| | - Xinghua Zhang
- College of Life Sciences, Wuhan University, Wuhan, China
| | - Zheng Liu
- TaiKang Center for Life and Medical Sciences, the Institute for Advanced Studies, Wuhan University, Wuhan, China.
- College of Life Sciences, Wuhan University, Wuhan, China.
| |
Collapse
|
10
|
Gong X, Nguyen R, Chen Z, Wen Z, Zhang X, Mak M. Volumetric Compression Shifts Rho GTPase Balance and Induces Mechanobiological Cell State Transition. BIORXIV : THE PREPRINT SERVER FOR BIOLOGY 2023:2023.10.08.561452. [PMID: 37873466 PMCID: PMC10592676 DOI: 10.1101/2023.10.08.561452] [Citation(s) in RCA: 1] [Impact Index Per Article: 1.0] [Reference Citation Analysis] [Abstract] [Track Full Text] [Subscribe] [Scholar Register] [Indexed: 10/25/2023]
Abstract
During development and disease progression, cells are subject to osmotic and mechanical stresses that modulate cell volume, which fundamentally influences cell homeostasis and has been linked to a variety of cellular functions. It is not well understood how the mechanobiological state of cells is programmed by the interplay of intracellular organization and complex extracellular mechanics when stimulated by cell volume modulation. Here, by controlling cell volume via osmotic pressure, we evaluate physical phenotypes (including cell shape, morphodynamics, traction force, and extracellular matrix (ECM) remodeling) and molecular signaling (YAP), and we uncover fundamental transitions in active biophysical states. We demonstrate that volumetric compression shifts the ratiometric balance of Rho GTPase activities, thereby altering mechanosensing and cytoskeletal organization in a reversible manner. Specifically, volumetric compression controls cell spreading, adhesion formation, and YAP nuclear translocation, while maintaining cell contractile activity. Furthermore, we show that on physiologically relevant fibrillar collagen I matrices, which are highly non-elastic, cells exhibit additional modes of cell volume-dependent mechanosensing that are not observable on elastic substrates. Notably, volumetric compression regulates the dynamics of cell-ECM interactions and irreversible ECM remodeling via Rac-directed protrusion dynamics, at both the single-cell level and the multicellular level. Our findings support that cell volume is a master biophysical regulator and reveal its roles in cell mechanical state transition, cell-ECM interactions, and biophysical tissue programming.
Collapse
|
11
|
Rajendran AK, Sankar D, Amirthalingam S, Kim HD, Rangasamy J, Hwang NS. Trends in mechanobiology guided tissue engineering and tools to study cell-substrate interactions: a brief review. Biomater Res 2023; 27:55. [PMID: 37264479 DOI: 10.1186/s40824-023-00393-8] [Citation(s) in RCA: 8] [Impact Index Per Article: 8.0] [Reference Citation Analysis] [Abstract] [Key Words] [Grants] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Received: 02/28/2023] [Accepted: 05/09/2023] [Indexed: 06/03/2023] Open
Abstract
Sensing the mechanical properties of the substrates or the matrix by the cells and the tissues, the subsequent downstream responses at the cellular, nuclear and epigenetic levels and the outcomes are beginning to get unraveled more recently. There have been various instances where researchers have established the underlying connection between the cellular mechanosignalling pathways and cellular physiology, cellular differentiation, and also tissue pathology. It has been now accepted that mechanosignalling, alone or in combination with classical pathways, could play a significant role in fate determination, development, and organization of cells and tissues. Furthermore, as mechanobiology is gaining traction, so do the various techniques to ponder and gain insights into the still unraveled pathways. This review would briefly discuss some of the interesting works wherein it has been shown that specific alteration of the mechanical properties of the substrates would lead to fate determination of stem cells into various differentiated cells such as osteoblasts, adipocytes, tenocytes, cardiomyocytes, and neurons, and how these properties are being utilized for the development of organoids. This review would also cover various techniques that have been developed and employed to explore the effects of mechanosignalling, including imaging of mechanosensing proteins, atomic force microscopy (AFM), quartz crystal microbalance with dissipation measurements (QCMD), traction force microscopy (TFM), microdevice arrays, Spatio-temporal image analysis, optical tweezer force measurements, mechanoscanning ion conductance microscopy (mSICM), acoustofluidic interferometric device (AID) and so forth. This review would provide insights to the researchers who work on exploiting various mechanical properties of substrates to control the cellular and tissue functions for tissue engineering and regenerative applications, and also will shed light on the advancements of various techniques that could be utilized to unravel the unknown in the field of cellular mechanobiology.
Collapse
Affiliation(s)
- Arun Kumar Rajendran
- School of Chemical and Biological Engineering, Institute of Chemical Processes, Seoul National University, Seoul, 08826, Republic of Korea
| | - Deepthi Sankar
- Polymeric Biomaterials Lab, School of Nanosciences and Molecular Medicine, Amrita Vishwa Vidyapeetham, Kochi, 682041, India
| | - Sivashanmugam Amirthalingam
- School of Chemical and Biological Engineering, Institute of Chemical Processes, Seoul National University, Seoul, 08826, Republic of Korea
- Institute of Engineering Research, Seoul National University, Seoul, 08826, Republic of Korea
| | - Hwan D Kim
- Department of Polymer Science and Engineering, Korea National University of Transportation, Chungju, 27469, Republic of Korea
- Department of Biomedical Engineering, Korea National University of Transportation, Chungju, 27469, Republic of Korea
| | - Jayakumar Rangasamy
- Polymeric Biomaterials Lab, School of Nanosciences and Molecular Medicine, Amrita Vishwa Vidyapeetham, Kochi, 682041, India.
| | - Nathaniel S Hwang
- School of Chemical and Biological Engineering, Institute of Chemical Processes, Seoul National University, Seoul, 08826, Republic of Korea.
- Institute of Engineering Research, Seoul National University, Seoul, 08826, Republic of Korea.
- Interdisciplinary Program in Bioengineering, Seoul National University, Seoul, 08826, Republic of Korea.
- Bio-MAX/N-Bio Institute, Institute of Bio-Engineering, Seoul National University, Seoul, 08826, Republic of Korea.
| |
Collapse
|
12
|
Nunes Vicente F, Chen T, Rossier O, Giannone G. Novel imaging methods and force probes for molecular mechanobiology of cytoskeleton and adhesion. Trends Cell Biol 2023; 33:204-220. [PMID: 36055943 DOI: 10.1016/j.tcb.2022.07.008] [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: 05/06/2022] [Revised: 07/26/2022] [Accepted: 07/27/2022] [Indexed: 12/01/2022]
Abstract
Detection and conversion of mechanical forces into biochemical signals is known as mechanotransduction. From cells to tissues, mechanotransduction regulates migration, proliferation, and differentiation in processes such as immune responses, development, and cancer progression. Mechanosensitive structures such as integrin adhesions, the actin cortex, ion channels, caveolae, and the nucleus sense and transmit forces. In vitro approaches showed that mechanosensing is based on force-dependent protein deformations and reorganizations. However, the mechanisms in cells remained unclear since cell imaging techniques lacked molecular resolution. Thanks to recent developments in super-resolution microscopy (SRM) and molecular force sensors, it is possible to obtain molecular insight of mechanosensing in live cells. We discuss how understanding of molecular mechanotransduction was revolutionized by these innovative approaches, focusing on integrin adhesions, actin structures, and the plasma membrane.
Collapse
Affiliation(s)
- Filipe Nunes Vicente
- University Bordeaux, CNRS, Interdisciplinary Institute for Neuroscience, IINS, UMR 5297, Bordeaux, France; Cell Biology and Biophysics Unit, European Molecular Biology Laboratory, Meyerhofstrasse 1, 69117 Heidelberg, Germany
| | - Tianchi Chen
- University Bordeaux, CNRS, Interdisciplinary Institute for Neuroscience, IINS, UMR 5297, Bordeaux, France
| | - Olivier Rossier
- University Bordeaux, CNRS, Interdisciplinary Institute for Neuroscience, IINS, UMR 5297, Bordeaux, France
| | - Grégory Giannone
- University Bordeaux, CNRS, Interdisciplinary Institute for Neuroscience, IINS, UMR 5297, Bordeaux, France.
| |
Collapse
|
13
|
Xu Y, Guo C, Yang X, Yuan W, Zhang X, Sun Y, Wen G, Wang L, Li H, Xiong C, Yang C. Super-resolution traction force microscopy with enhanced tracer density enables capturing molecular scale traction. Biomater Sci 2023; 11:1056-1065. [PMID: 36562450 DOI: 10.1039/d2bm01332k] [Citation(s) in RCA: 0] [Impact Index Per Article: 0] [Reference Citation Analysis] [Abstract] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Indexed: 12/24/2022]
Abstract
Cell traction mediates the biochemical and mechanical interactions between the cell and its extracellular matrix (ECM). Traction force microscopy (TFM) is a powerful technique for quantitative cellular scale traction analysis. However, it is challenging to characterize macromolecular scale traction events with current TFM due to the limited sampling density and algorithmic precision. In this article, we introduce a super-resolution TFM by utilizing a novel substrate surface modification method. Our TFM technique achieved a spatial resolution comparable to fluorescence microscopy and precision comparable to the rupture force of an integrin-ligand bond. Correlated imaging of TFM with fluorescence microscopy demonstrated that the residing paxillin highly correlated with traction while α5 integrin was located differently. Time-lapse TFM imaging captured a transient traction variation as the adhesion protein passed by. Thus, the novel super-resolution TFM benefits the studies on cellular biochemical and mechanical interactions.
Collapse
Affiliation(s)
- Yue Xu
- Institute of Biomechanics and Medical Engineering, School of Aerospace Engineering, Tsinghua University, Beijing 10084, People's Republic of China.
| | - Chuanwen Guo
- Institute of Biomechanics and Medical Engineering, School of Aerospace Engineering, Tsinghua University, Beijing 10084, People's Republic of China.
| | - Xueyi Yang
- Institute of Biomechanics and Medical Engineering, School of Aerospace Engineering, Tsinghua University, Beijing 10084, People's Republic of China.
| | - Weihong Yuan
- State Key Laboratory of Membrane Biology, Biodynamic Optical Imaging Centre (BIOPIC), School of Life Sciences, Peking University, Beijing 100871, China
| | - Xu Zhang
- Institute of Biomechanics and Medical Engineering, School of Aerospace Engineering, Tsinghua University, Beijing 10084, People's Republic of China.
| | - Yujie Sun
- State Key Laboratory of Membrane Biology, Biodynamic Optical Imaging Centre (BIOPIC), School of Life Sciences, Peking University, Beijing 100871, China
| | - Gang Wen
- Jiangsu Key Laboratory of Medical Optics, Suzhou Institute of Biomedical Engineering and Technology, Chinese Academy of Sciences, Suzhou, Jiangsu 215163, China.
| | - Linbo Wang
- Jiangsu Key Laboratory of Medical Optics, Suzhou Institute of Biomedical Engineering and Technology, Chinese Academy of Sciences, Suzhou, Jiangsu 215163, China.
| | - Hui Li
- Jiangsu Key Laboratory of Medical Optics, Suzhou Institute of Biomedical Engineering and Technology, Chinese Academy of Sciences, Suzhou, Jiangsu 215163, China.
| | - Chunyang Xiong
- State Key Laboratory for Turbulence and Complex System, and Department of Mechanics and Engineering Science, College of Engineering, Academy for Advanced Interdisciplinary Studies, Peking University, Beijing 100871, People's Republic of China.
| | - Chun Yang
- Institute of Biomechanics and Medical Engineering, School of Aerospace Engineering, Tsinghua University, Beijing 10084, People's Republic of China.
| |
Collapse
|
14
|
Scott S, Weiss M, Selhuber-Unkel C, Barooji YF, Sabri A, Erler JT, Metzler R, Oddershede LB. Extracting, quantifying, and comparing dynamical and biomechanical properties of living matter through single particle tracking. Phys Chem Chem Phys 2023; 25:1513-1537. [PMID: 36546878 DOI: 10.1039/d2cp01384c] [Citation(s) in RCA: 0] [Impact Index Per Article: 0] [Reference Citation Analysis] [Abstract] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Indexed: 12/24/2022]
Abstract
A panoply of new tools for tracking single particles and molecules has led to an explosion of experimental data, leading to novel insights into physical properties of living matter governing cellular development and function, health and disease. In this Perspective, we present tools to investigate the dynamics and mechanics of living systems from the molecular to cellular scale via single-particle techniques. In particular, we focus on methods to measure, interpret, and analyse complex data sets that are associated with forces, materials properties, transport, and emergent organisation phenomena within biological and soft-matter systems. Current approaches, challenges, and existing solutions in the associated fields are outlined in order to support the growing community of researchers at the interface of physics and the life sciences. Each section focuses not only on the general physical principles and the potential for understanding living matter, but also on details of practical data extraction and analysis, discussing limitations, interpretation, and comparison across different experimental realisations and theoretical frameworks. Particularly relevant results are introduced as examples. While this Perspective describes living matter from a physical perspective, highlighting experimental and theoretical physics techniques relevant for such systems, it is also meant to serve as a solid starting point for researchers in the life sciences interested in the implementation of biophysical methods.
Collapse
Affiliation(s)
- Shane Scott
- Institute of Physiology, Kiel University, Hermann-Rodewald-Straße 5, 24118 Kiel, Germany
| | - Matthias Weiss
- Experimental Physics I, University of Bayreuth, Universitätsstr. 30, D-95447 Bayreuth, Germany
| | - Christine Selhuber-Unkel
- Institute for Molecular Systems Engineering, Heidelberg University, D-69120 Heidelberg, Germany.,Max Planck School Matter to Life, Jahnstraße 29, D-69120 Heidelberg, Germany
| | - Younes F Barooji
- Niels Bohr Institute, Blegdamsvej 17, DK-2100 Copenhagen, Denmark.
| | - Adal Sabri
- Experimental Physics I, University of Bayreuth, Universitätsstr. 30, D-95447 Bayreuth, Germany
| | - Janine T Erler
- BRIC, University of Copenhagen, Ole Maaløes Vej 5, DK-2200 Copenhagen, Denmark.
| | - Ralf Metzler
- Institute of Physics and Astronomy, University of Potsdam, Karl-Liebknecht Str. 24/25, D-14476 Potsdam, Germany.,Asia Pacific Center for Theoretical Physics, Pohang 37673, Republic of Korea
| | | |
Collapse
|
15
|
Afzal J, Du W, Novin A, Liu Y, Wali K, Murthy A, Garen A, Wagner G. Paracrine HB-EGF signaling reduce enhanced contractile and energetic state of activated decidual fibroblasts by rebalancing SRF-MRTF-TCF transcriptional axis. Front Cell Dev Biol 2022; 10:927631. [PMID: 36147738 PMCID: PMC9485834 DOI: 10.3389/fcell.2022.927631] [Citation(s) in RCA: 7] [Impact Index Per Article: 3.5] [Reference Citation Analysis] [Abstract] [Grants] [Track Full Text] [Download PDF] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Received: 04/24/2022] [Accepted: 08/09/2022] [Indexed: 11/26/2022] Open
Abstract
Multiple parallels exist between placentation and cancer dissemination at molecular, cellular, and anatomical levels, presenting placentation as a unique model to mechanistically understand the onset of cancer metastasis. In humans, interaction of placenta and the endometrium results eventually in deep invasion of placental extravillous trophoblasts (EVTs) into the maternal stroma, a process similar to stromal trespass by disseminating carcinoma cells. In anticipation of implantation, endometrial fibroblasts (ESFs) undergo a process called decidualization during the secretory phase of the menstrual cycle. Decidualization, among other substantial changes associated with ESF differentiation, also involves a component of fibroblast activation, and myofibroblast transformation. Here, using traction force microscopy, we show that increased cellular contractility in decidualized ESFs is reversed after interaction with EVTs. We also report here the large changes in energetic state of ESFs upon decidualization, showing increased oxidative phosphorylation, mitochondrial competency and ATP generation, as well as enhanced aerobic glycolysis, presenting mechanical contractility and energetic state as new functional hallmarks for decidualization. These energetic changes accompanying the marked increase in contractile force generation in decidualization were reduced in the presence of EVTs. We also show that increase in decidual contractility and mechanical resistance to invasion is achieved by SRF-MRTF transcriptional activation, achieved via increased phosphorylation of fibroblast-specific myosin light chain 9 (MYL9). EVT induced paracrine secretion of Heparin Binding Epidermal Growth Factor (HBEGF), a potent MAPK activator, which shifts the balance of SRF association away from MRTF based transcription, reducing decidual ESF contractility and mechanical resistance to placental invasion. Our results identify a new axis of intercellular communication in the placental bed modulating stromal force generation and resistance to invasion with concurrent downregulation of cellular energetics. These findings have important implications for implantation related disorders, as well as stromal control of cancer dissemination.
Collapse
Affiliation(s)
- Junaid Afzal
- Division of Cardiology, Department of Medicine, University of California San Francisco, San Francisco, CA, United States
- *Correspondence: Junaid Afzal, ; Kshitiz,
| | - Wenqiang Du
- Department of Biomedical Engineering, University of Connecticut Health, Farmington, CT, United States
| | - Ashkan Novin
- Department of Biomedical Engineering, University of Connecticut Health, Farmington, CT, United States
| | - Yamin Liu
- Department of Biomedical Engineering, University of Connecticut Health, Farmington, CT, United States
| | - Khadija Wali
- Department of Biomedical Engineering, University of Connecticut Health, Farmington, CT, United States
| | - Anarghya Murthy
- Department of Biomedical Engineering, University of Connecticut Health, Farmington, CT, United States
| | - Ashley Garen
- Department of Biomedical Engineering, University of Connecticut Health, Farmington, CT, United States
| | - Gunter Wagner
- Department of Ecology and Evolution, Yale University West Campus, West Haven, CT, United States
- Systems Biology Institute, Yale University, West Haven, CT, United States
| |
Collapse
|
16
|
Mustapha F, Sengupta K, Puech PH. May the force be with your (immune) cells: an introduction to traction force microscopy in Immunology. Front Immunol 2022; 13:898558. [PMID: 35990636 PMCID: PMC9389945 DOI: 10.3389/fimmu.2022.898558] [Citation(s) in RCA: 0] [Impact Index Per Article: 0] [Reference Citation Analysis] [Abstract] [Key Words] [MESH Headings] [Track Full Text] [Download PDF] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Received: 03/17/2022] [Accepted: 06/28/2022] [Indexed: 11/21/2022] Open
Abstract
For more than a couple of decades now, "force" has been recognized as an important physical parameter that cells employ to adapt to their microenvironment. Whether it is externally applied, or internally generated, cells use force to modulate their various actions, from adhesion and migration to differentiation and immune function. T lymphocytes use such mechano-sensitivity to decipher signals when recognizing cognate antigens presented on the surface of antigen presenting cells (APCs), a critical process in the adaptive immune response. As such, many techniques have been developed and used to measure the forces felt/exerted by these small, solitary and extremely reactive cells to decipher their influence on diverse T cell functions, primarily activation. Here, we focus on traction force microscopy (TFM), in which a deformable substrate, coated with the appropriate molecules, acts as a force sensor on the cellular scale. This technique has recently become a center of interest for many groups in the "ImmunoBiophysics" community and, as a consequence, has been subjected to refinements for its application to immune cells. Here, we present an overview of TFM, the precautions and pitfalls, and the most recent developments in the context of T cell immunology.
Collapse
Affiliation(s)
- Farah Mustapha
- Laboratory Adhesion Inflammation (LAI), INSERM, CNRS, Aix Marseille University, Marseille, France
- Centre Interdisciplinaire de Nanoscience de Marseille (CINaM), CNRS, Aix Marseille University, Marseille, France
- Turing Center for Living Systems (CENTURI), Marseille, France
| | - Kheya Sengupta
- Centre Interdisciplinaire de Nanoscience de Marseille (CINaM), CNRS, Aix Marseille University, Marseille, France
- Turing Center for Living Systems (CENTURI), Marseille, France
| | - Pierre-Henri Puech
- Laboratory Adhesion Inflammation (LAI), INSERM, CNRS, Aix Marseille University, Marseille, France
- Turing Center for Living Systems (CENTURI), Marseille, France
| |
Collapse
|
17
|
Colin-York H, Heddleston J, Wait E, Karedla N, deSantis M, Khuon S, Chew TL, Sbalzarini IF, Fritzsche M. Quantifying Molecular Dynamics within Complex Cellular Morphologies using LLSM-FRAP. SMALL METHODS 2022; 6:e2200149. [PMID: 35344286 DOI: 10.1002/smtd.202200149] [Citation(s) in RCA: 1] [Impact Index Per Article: 0.5] [Reference Citation Analysis] [Abstract] [Key Words] [MESH Headings] [Track Full Text] [Subscribe] [Scholar Register] [Received: 02/01/2022] [Indexed: 06/14/2023]
Abstract
Quantifying molecular dynamics within the context of complex cellular morphologies is essential toward understanding the inner workings and function of cells. Fluorescence recovery after photobleaching (FRAP) is one of the most broadly applied techniques to measure the reaction diffusion dynamics of molecules in living cells. FRAP measurements typically restrict themselves to single-plane image acquisition within a subcellular-sized region of interest due to the limited temporal resolution and undesirable photobleaching induced by 3D fluorescence confocal or widefield microscopy. Here, an experimental and computational pipeline combining lattice light sheet microscopy, FRAP, and numerical simulations, offering rapid and minimally invasive quantification of molecular dynamics with respect to 3D cell morphology is presented. Having the opportunity to accurately measure and interpret the dynamics of molecules in 3D with respect to cell morphology has the potential to reveal unprecedented insights into the function of living cells.
Collapse
Affiliation(s)
- Huw Colin-York
- MRC Human Immunology Unit, Weatherall Institute of Molecular Medicine, University of Oxford, Oxford, OX3 9DS, UK
- Kennedy Institute for Rheumatology, University of Oxford, Oxford, OX3 7LF, UK
| | - John Heddleston
- Howard Hughes Medical Institute, Janelia Research Campus, Ashburn, VA 20147, USA
| | - Eric Wait
- Howard Hughes Medical Institute, Janelia Research Campus, Ashburn, VA 20147, USA
| | - Narain Karedla
- Rosalind Franklin Institute, Harwell Campus, Didcot, OX11 0FA, UK
| | - Michael deSantis
- Howard Hughes Medical Institute, Janelia Research Campus, Ashburn, VA 20147, USA
| | - Satya Khuon
- Howard Hughes Medical Institute, Janelia Research Campus, Ashburn, VA 20147, USA
| | - Teng-Leong Chew
- Howard Hughes Medical Institute, Janelia Research Campus, Ashburn, VA 20147, USA
| | - Ivo F Sbalzarini
- Faculty of Computer Science, Technische Universität Dresden, 01187, Dresden, Germany
- Max Planck Institute of Molecular Cell Biology and Genetics, 01307, Dresden, Germany
| | - Marco Fritzsche
- MRC Human Immunology Unit, Weatherall Institute of Molecular Medicine, University of Oxford, Oxford, OX3 9DS, UK
- Kennedy Institute for Rheumatology, University of Oxford, Oxford, OX3 7LF, UK
- Rosalind Franklin Institute, Harwell Campus, Didcot, OX11 0FA, UK
| |
Collapse
|
18
|
Duan X, Huang J. Deep learning-based 3D cellular force reconstruction directly from volumetric images. Biophys J 2022; 121:2180-2192. [PMID: 35484854 DOI: 10.1016/j.bpj.2022.04.028] [Citation(s) in RCA: 0] [Impact Index Per Article: 0] [Reference Citation Analysis] [Abstract] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Received: 11/10/2021] [Revised: 03/26/2022] [Accepted: 04/22/2022] [Indexed: 11/28/2022] Open
Abstract
The forces exerted by single cells in the three-dimensional (3D) environments play a crucial role in modulating cellular functions and behaviors closely related to physiological and pathological processes. Cellular force microscopy (CFM) provides a feasible solution for quantifying the mechanical interactions, which usually regains cellular forces from deformation information of extracellular matrices embedded with fluorescent beads. Owing to computational complexity, the traditional 3D-CFM is usually extremely time-consuming, which makes it challenging for efficient force recovery and large-scale sample analysis. With the aid of deep neural networks, this study puts forward a novel data-driven 3D-CFM to reconstruct 3D cellular force fields directly from volumetric images with random fluorescence patterns. The deep learning (DL)-based network is established through stacking deep convolutional neural network (DCNN) and specific function layers. Some necessary physical information associated with constitutive relation of extracellular matrix material is coupled to the data-driven network. The mini-batch stochastic gradient descent and back-propagation algorithms are introduced to ensure its convergence and training efficiency. The network not only have good generalization ability and robustness, but also can recover 3D cellular forces directly from the input fluorescence image pairs. Particularly, the computational efficiency of the DL-based network is at least one to two orders of magnitude higher than that of the traditional 3D-CFM. This study provides a novel scheme for developing high-performance 3D cellular force microscopy to quantitatively characterize mechanical interactions between single cells and surrounding extracellular matrices, which is of vital importance for quantitative investigations in biomechanics and mechanobiology.
Collapse
Affiliation(s)
- Xiaocen Duan
- Department of Mechanics and Engineering Science, College of Engineering, Peking University, Beijing 100871, China;; Academy for Advanced Interdisciplinary Studies, Peking University, Beijing 100871, China
| | - Jianyong Huang
- Department of Mechanics and Engineering Science, College of Engineering, Peking University, Beijing 100871, China;; Beijing Innovation Center for Engineering Science and Advanced Technology, College of Engineering, Peking University, Beijing 100871, China.
| |
Collapse
|
19
|
A vasculature niche orchestrates stromal cell phenotype through PDGF signaling: Importance in human fibrotic disease. Proc Natl Acad Sci U S A 2022; 119:e2120336119. [PMID: 35320046 PMCID: PMC9060460 DOI: 10.1073/pnas.2120336119] [Citation(s) in RCA: 11] [Impact Index Per Article: 5.5] [Reference Citation Analysis] [Abstract] [Key Words] [Track Full Text] [Download PDF] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Indexed: 02/06/2023] Open
Abstract
Tissue fibrotic diseases, for example of the liver and lung, represent a huge unmet medical need. In this study, using single-cell RNA sequencing, cytometry by time of flight (CyTOF), tissue imaging, and functional assays, we identify a complex vascular niche in Dupuytren’s disease (DD), a common localized fibrotic condition of the palm, where early-disease-stage tissue can be accessed readily. We uncover a population of myofibroblast precursors within the pericyte compartment and demonstrate that the endothelium instructs the differentiation of functionally distinct stromal cells, thereby orchestrating discrete microenvironments in the fibrotic milieu. Together, these findings provide a basis for the concept of targeting blood vessel signaling to control the progression of human fibrosis. Fibrosis is characterized by excessive matrix protein accumulation and contributes to significant morbidity and mortality in the Western world. The relative lack of effective antifibrotic therapeutics for the majority of these conditions reflects the difficulty in identifying targets for human fibrosis. Animal models fail to recapitulate all of the facets of human disease, and the limited clinical samples from patients with fibrosis of visceral organs are usually of late-stage disease [J. Nanchahal, B. Hinz, Proc. Natl. Acad. Sci. U.S.A. 113, 7291–7293 (2016)]. Here, we use Dupuytren’s disease (DD), a localized fibrotic condition of the hand, as a model to profile the vasculature niche of human fibrosis at single-cell resolution. Our spatially resolved molecular taxonomy of fibrotic blood vessels identifies distinct endothelial and pericyte populations and demonstrates a complex topological organization in the fibrotic microenvironment. In developing fibrosis, we show that the endothelium acts to promote immune regulatory fibroblast phenotype through platelet-derived growth factor (PDGF) signaling, thereby sustaining an immune cell–enriched perivascular niche. Moreover, we highlight pericytes as “housing” a putative myofibroblast precursor in DD. Overall, our results elucidate a tightly coupled vasculature niche in fibrosis that instructs the differentiation of functionally distinct stromal cells. These findings provide an important translational resource and highlight the therapeutic potential of targeting blood vessel signaling in human fibrosis.
Collapse
|
20
|
Mgharbel A, Migdal C, Bouchonville N, Dupenloup P, Fuard D, Lopez-Soler E, Tomba C, Courçon M, Gulino-Debrac D, Delanoë-Ayari H, Nicolas A. Cells on Hydrogels with Micron-Scaled Stiffness Patterns Demonstrate Local Stiffness Sensing. NANOMATERIALS (BASEL, SWITZERLAND) 2022; 12:648. [PMID: 35214978 PMCID: PMC8880377 DOI: 10.3390/nano12040648] [Citation(s) in RCA: 1] [Impact Index Per Article: 0.5] [Reference Citation Analysis] [Abstract] [Key Words] [Grants] [Track Full Text] [Download PDF] [Figures] [Subscribe] [Scholar Register] [Received: 01/10/2022] [Revised: 01/31/2022] [Accepted: 02/07/2022] [Indexed: 12/15/2022]
Abstract
Cell rigidity sensing-a basic cellular process allowing cells to adapt to mechanical cues-involves cell capabilities exerting force on the extracellular environment. In vivo, cells are exposed to multi-scaled heterogeneities in the mechanical properties of the surroundings. Here, we investigate whether cells are able to sense micron-scaled stiffness textures by measuring the forces they transmit to the extracellular matrix. To this end, we propose an efficient photochemistry of polyacrylamide hydrogels to design micron-scale stiffness patterns with kPa/µm gradients. Additionally, we propose an original protocol for the surface coating of adhesion proteins, which allows tuning the surface density from fully coupled to fully independent of the stiffness pattern. This evidences that cells pull on their surroundings by adjusting the level of stress to the micron-scaled stiffness. This conclusion was achieved through improvements in the traction force microscopy technique, e.g., adapting to substrates with a non-uniform stiffness and achieving a submicron resolution thanks to the implementation of a pyramidal optical flow algorithm. These developments provide tools for enhancing the current understanding of the contribution of stiffness alterations in many pathologies, including cancer.
Collapse
Affiliation(s)
- Abbas Mgharbel
- University Grenoble Alps, CNRS, LTM, 38000 Grenoble, France; (A.M.); (C.M.); (N.B.); (P.D.); (D.F.); (E.L.-S.); (C.T.)
- University Grenoble Alps, CEA, CNRS, Inserm, BIG-BCI, 38000 Grenoble, France; (M.C.); (D.G.-D.)
| | - Camille Migdal
- University Grenoble Alps, CNRS, LTM, 38000 Grenoble, France; (A.M.); (C.M.); (N.B.); (P.D.); (D.F.); (E.L.-S.); (C.T.)
- University Grenoble Alps, CEA, CNRS, Inserm, BIG-BCI, 38000 Grenoble, France; (M.C.); (D.G.-D.)
| | - Nicolas Bouchonville
- University Grenoble Alps, CNRS, LTM, 38000 Grenoble, France; (A.M.); (C.M.); (N.B.); (P.D.); (D.F.); (E.L.-S.); (C.T.)
| | - Paul Dupenloup
- University Grenoble Alps, CNRS, LTM, 38000 Grenoble, France; (A.M.); (C.M.); (N.B.); (P.D.); (D.F.); (E.L.-S.); (C.T.)
| | - David Fuard
- University Grenoble Alps, CNRS, LTM, 38000 Grenoble, France; (A.M.); (C.M.); (N.B.); (P.D.); (D.F.); (E.L.-S.); (C.T.)
| | - Eline Lopez-Soler
- University Grenoble Alps, CNRS, LTM, 38000 Grenoble, France; (A.M.); (C.M.); (N.B.); (P.D.); (D.F.); (E.L.-S.); (C.T.)
- University Grenoble Alps, CEA, CNRS, Inserm, BIG-BCI, 38000 Grenoble, France; (M.C.); (D.G.-D.)
| | - Caterina Tomba
- University Grenoble Alps, CNRS, LTM, 38000 Grenoble, France; (A.M.); (C.M.); (N.B.); (P.D.); (D.F.); (E.L.-S.); (C.T.)
- University Grenoble Alps, CNRS, Grenoble INP, Institut Néel, 38000 Grenoble, France
| | - Marie Courçon
- University Grenoble Alps, CEA, CNRS, Inserm, BIG-BCI, 38000 Grenoble, France; (M.C.); (D.G.-D.)
| | - Danielle Gulino-Debrac
- University Grenoble Alps, CEA, CNRS, Inserm, BIG-BCI, 38000 Grenoble, France; (M.C.); (D.G.-D.)
| | - Héléne Delanoë-Ayari
- Université de Lyon, University Claude Bernard Lyon1, CNRS, Institut Lumière Matière, 69622 Villeurbanne, France;
| | - Alice Nicolas
- University Grenoble Alps, CNRS, LTM, 38000 Grenoble, France; (A.M.); (C.M.); (N.B.); (P.D.); (D.F.); (E.L.-S.); (C.T.)
| |
Collapse
|
21
|
Carvalho E, Morais M, Ferreira H, Silva M, Guimarães S, Pêgo A. A paradigm shift: Bioengineering meets mechanobiology towards overcoming remyelination failure. Biomaterials 2022; 283:121427. [DOI: 10.1016/j.biomaterials.2022.121427] [Citation(s) in RCA: 2] [Impact Index Per Article: 1.0] [Reference Citation Analysis] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Received: 05/28/2021] [Revised: 01/31/2022] [Accepted: 02/17/2022] [Indexed: 12/14/2022]
|
22
|
van Santen VJB, Klein-Nulend J, Bakker AD, Jaspers RT. Stiff matrices enhance myoblast proliferation, reduce differentiation, and alter the response to fluid shear stress in vitro. Cell Biochem Biophys 2022; 80:161-170. [DOI: 10.1007/s12013-021-01050-4] [Citation(s) in RCA: 0] [Impact Index Per Article: 0] [Reference Citation Analysis] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Accepted: 11/18/2021] [Indexed: 11/03/2022]
|
23
|
Gil-Redondo JC, Weber A, Zbiral B, Vivanco MDM, Toca-Herrera JL. Substrate stiffness modulates the viscoelastic properties of MCF-7 cells. J Mech Behav Biomed Mater 2021; 125:104979. [PMID: 34826769 DOI: 10.1016/j.jmbbm.2021.104979] [Citation(s) in RCA: 8] [Impact Index Per Article: 2.7] [Reference Citation Analysis] [Abstract] [Key Words] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Received: 08/04/2021] [Revised: 10/27/2021] [Accepted: 11/12/2021] [Indexed: 01/01/2023]
Abstract
Cells sense stiffness of surrounding tissues and adapt their activity, proliferation, motility and mechanical properties based on such interactions. Cells probe the stiffness of the substrate by anchoring and pulling to their surroundings, transmitting force to the extracellular matrix and other cells, and respond to the resistance they sense, mainly through changes in their cytoskeleton. Cancer and other diseases alter stiffness of tissues, and the response of cancer cells to this stiffness can also be affected. In the present study we show that MCF-7 breast cancer cells seeded on polyacrylamide gels have the ability to detect the stiffness of the substrate and alter their mechanical properties in response. MCF-7 cells plated on soft substrates display lower stiffness and viscosity when compared to those seeded on stiffer gels or glass. These differences can be associated with differences in the morphology and cytoskeleton organisation, since cells seeded on soft substrates have a round morphology, while cells seeded on stiffer substrates acquire a flat and spread morphology with formation of actin filaments, similar to that observed when seeded on glass. These findings show that MCF-7 cells can detect the stiffness of the surrounding microenvironment and thus, modify their mechanical properties.
Collapse
Affiliation(s)
- Juan Carlos Gil-Redondo
- Institute of Biophysics, Department of Nanobiotechnology, University of Natural Resources and Life Sciences Vienna, Muthgasse 11, 1190, Vienna, Austria.
| | - Andreas Weber
- Institute of Biophysics, Department of Nanobiotechnology, University of Natural Resources and Life Sciences Vienna, Muthgasse 11, 1190, Vienna, Austria.
| | - Barbara Zbiral
- Institute of Biophysics, Department of Nanobiotechnology, University of Natural Resources and Life Sciences Vienna, Muthgasse 11, 1190, Vienna, Austria.
| | - Maria dM Vivanco
- Cancer Heterogeneity Lab, CIC BioGUNE, Basque Research and Technology Alliance, BRTA, Bizkaia Technology Park, 48160, Derio, Spain.
| | - José L Toca-Herrera
- Institute of Biophysics, Department of Nanobiotechnology, University of Natural Resources and Life Sciences Vienna, Muthgasse 11, 1190, Vienna, Austria.
| |
Collapse
|
24
|
Korobchevskaya K, Colin-York H, Barbieri L, Fritzsche M. Extended mechanical force measurements using structured illumination microscopy. PHILOSOPHICAL TRANSACTIONS. SERIES A, MATHEMATICAL, PHYSICAL, AND ENGINEERING SCIENCES 2021; 379:20200151. [PMID: 33896200 PMCID: PMC7612033 DOI: 10.1098/rsta.2020.0151] [Citation(s) in RCA: 0] [Impact Index Per Article: 0] [Reference Citation Analysis] [Abstract] [Key Words] [MESH Headings] [Grants] [Track Full Text] [Subscribe] [Scholar Register] [Accepted: 01/11/2021] [Indexed: 06/12/2023]
Abstract
Quantifying cell generated mechanical forces is key to furthering our understanding of mechanobiology. Traction force microscopy (TFM) is one of the most broadly applied force probing technologies, but its sensitivity is strictly dependent on the spatio-temporal resolution of the underlying imaging system. In previous works, it was demonstrated that increased sampling densities of cell derived forces permitted by super-resolution fluorescence imaging enhanced the sensitivity of the TFM method. However, these recent advances to TFM based on super-resolution techniques were limited to slow acquisition speeds and high illumination powers. Here, we present three novel TFM approaches that, in combination with total internal reflection, structured illumination microscopy and astigmatism, improve the spatial and temporal performance in either two-dimensional or three-dimensional mechanical force quantification, while maintaining low illumination powers. These three techniques can be straightforwardly implemented on a single optical set-up offering a powerful platform to provide new insights into the physiological force generation in a wide range of biological studies. This article is part of the Theo Murphy meeting issue 'Super-resolution structured illumination microscopy (part 1)'.
Collapse
Affiliation(s)
- Kseniya Korobchevskaya
- Kennedy Institute for Rheumatology, Roosevelt Drive, University of Oxford, Oxford, OX3 7LF, United Kingdom
| | - Huw Colin-York
- Kennedy Institute for Rheumatology, Roosevelt Drive, University of Oxford, Oxford, OX3 7LF, United Kingdom
| | - Liliana Barbieri
- MRC Human Immunology Unit, Weatherall Institute of Molecular Medicine, University of Oxford, Headley Way, Oxford. OX3 9DS, United Kingdom
| | - Marco Fritzsche
- Kennedy Institute for Rheumatology, Roosevelt Drive, University of Oxford, Oxford, OX3 7LF, United Kingdom
- MRC Human Immunology Unit, Weatherall Institute of Molecular Medicine, University of Oxford, Headley Way, Oxford. OX3 9DS, United Kingdom
- Rosalind Franklin Institute, Harwell Campus, Didcot, OX11 0FA, United Kingdom
| |
Collapse
|
25
|
Mishra YG, Manavathi B. Focal adhesion dynamics in cellular function and disease. Cell Signal 2021; 85:110046. [PMID: 34004332 DOI: 10.1016/j.cellsig.2021.110046] [Citation(s) in RCA: 65] [Impact Index Per Article: 21.7] [Reference Citation Analysis] [Abstract] [Key Words] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Received: 04/30/2021] [Accepted: 05/13/2021] [Indexed: 02/06/2023]
Abstract
Acting as a bridge between the cytoskeleton of the cell and the extra cellular matrix (ECM), the cell-ECM adhesions with integrins at their core, play a major role in cell signalling to direct mechanotransduction, cell migration, cell cycle progression, proliferation, differentiation, growth and repair. Biochemically, these adhesions are composed of diverse, yet an organised group of structural proteins, receptors, adaptors, various enzymes including protein kinases, phosphatases, GTPases, proteases, etc. as well as scaffolding molecules. The major integrin adhesion complexes (IACs) characterised are focal adhesions (FAs), invadosomes (podosomes and invadopodia), hemidesmosomes (HDs) and reticular adhesions (RAs). The varied composition and regulation of the IACs and their signalling, apart from being an integral part of normal cell survival, has been shown to be of paramount importance in various developmental and pathological processes. This review per-illustrates the recent advancements in the research of IACs, their crucial roles in normal as well as diseased states. We have also touched on few of the various methods that have been developed over the years to visualise IACs, measure the forces they exert and study their signalling and molecular composition. Having such pertinent roles in the context of various pathologies, these IACs need to be understood and studied to develop therapeutical targets. We have given an update to the studies done in recent years and described various techniques which have been applied to study these structures, thereby, providing context in furthering research with respect to IAC targeted therapeutics.
Collapse
Affiliation(s)
- Yasaswi Gayatri Mishra
- Department of Biochemistry, School of Life Sciences, University of Hyderabad, Hyderabad 500046, India
| | - Bramanandam Manavathi
- Department of Biochemistry, School of Life Sciences, University of Hyderabad, Hyderabad 500046, India.
| |
Collapse
|
26
|
Zheng Q, Peng M, Liu Z, Li S, Han R, Ouyang H, Fan Y, Pan C, Hu W, Zhai J, Li Z, Wang ZL. Dynamic real-time imaging of living cell traction force by piezo-phototronic light nano-antenna array. SCIENCE ADVANCES 2021; 7:7/22/eabe7738. [PMID: 34039600 PMCID: PMC8153726 DOI: 10.1126/sciadv.abe7738] [Citation(s) in RCA: 31] [Impact Index Per Article: 10.3] [Reference Citation Analysis] [Abstract] [Grants] [Track Full Text] [Subscribe] [Scholar Register] [Received: 09/14/2020] [Accepted: 04/08/2021] [Indexed: 05/24/2023]
Abstract
Dynamic mapping of the cell-generated force of cardiomyocytes will help provide an intrinsic understanding of the heart. However, a real-time, dynamic, and high-resolution mapping of the force distribution across a single living cell remains a challenge. Here, we established a force mapping method based on a "light nano-antenna" array with the use of piezo-phototronic effect. A spatial resolution of 800 nm and a temporal resolution of 333 ms have been demonstrated for force mapping. The dynamic mapping of cell force of live cardiomyocytes was directly derived by locating the antennas' positions and quantifying the light intensities of the piezo-phototronic light nano-antenna array. This study presents a rapid and ultrahigh-resolution methodology for the fundamental study of cardiomyocyte behavior at the cell or subcellular level. It can provide valuable information about disease detection, drug screening, and tissue engineering for heart-related studies.
Collapse
Affiliation(s)
- Qiang Zheng
- CAS Center for Excellence in Nanoscience, Beijing Key Laboratory of Micro-Nano Energy and Sensor, Beijing Institute of Nanoenergy and Nanosystems, Chinese Academy of Sciences, 100083 Beijing, China
| | - Mingzeng Peng
- CAS Center for Excellence in Nanoscience, Beijing Key Laboratory of Micro-Nano Energy and Sensor, Beijing Institute of Nanoenergy and Nanosystems, Chinese Academy of Sciences, 100083 Beijing, China
| | - Zhuo Liu
- CAS Center for Excellence in Nanoscience, Beijing Key Laboratory of Micro-Nano Energy and Sensor, Beijing Institute of Nanoenergy and Nanosystems, Chinese Academy of Sciences, 100083 Beijing, China
- Beijing Advanced Innovation Center for Biomedical Engineering, Key Laboratory for Biomechanics and Mechanobiology of Ministry of Education, School of Biological Science and Medical Engineering, Beihang University, 100191 Beijing, China
| | - Shuyu Li
- Beijing Advanced Innovation Center for Biomedical Engineering, Key Laboratory for Biomechanics and Mechanobiology of Ministry of Education, School of Biological Science and Medical Engineering, Beihang University, 100191 Beijing, China
| | - Rongcheng Han
- Institute of Genetics and Developmental Biology, Chinese Academy of Sciences, 100101 Beijing, China
| | - Han Ouyang
- CAS Center for Excellence in Nanoscience, Beijing Key Laboratory of Micro-Nano Energy and Sensor, Beijing Institute of Nanoenergy and Nanosystems, Chinese Academy of Sciences, 100083 Beijing, China
- Beijing Advanced Innovation Center for Biomedical Engineering, Key Laboratory for Biomechanics and Mechanobiology of Ministry of Education, School of Biological Science and Medical Engineering, Beihang University, 100191 Beijing, China
| | - Yubo Fan
- Beijing Advanced Innovation Center for Biomedical Engineering, Key Laboratory for Biomechanics and Mechanobiology of Ministry of Education, School of Biological Science and Medical Engineering, Beihang University, 100191 Beijing, China
| | - Caofeng Pan
- CAS Center for Excellence in Nanoscience, Beijing Key Laboratory of Micro-Nano Energy and Sensor, Beijing Institute of Nanoenergy and Nanosystems, Chinese Academy of Sciences, 100083 Beijing, China
- School of Nanoscience and Technology, University of Chinese Academy of Sciences, 100049 Beijing, China
| | - Weiguo Hu
- CAS Center for Excellence in Nanoscience, Beijing Key Laboratory of Micro-Nano Energy and Sensor, Beijing Institute of Nanoenergy and Nanosystems, Chinese Academy of Sciences, 100083 Beijing, China
- School of Nanoscience and Technology, University of Chinese Academy of Sciences, 100049 Beijing, China
| | - Junyi Zhai
- CAS Center for Excellence in Nanoscience, Beijing Key Laboratory of Micro-Nano Energy and Sensor, Beijing Institute of Nanoenergy and Nanosystems, Chinese Academy of Sciences, 100083 Beijing, China.
- School of Nanoscience and Technology, University of Chinese Academy of Sciences, 100049 Beijing, China
| | - Zhou Li
- CAS Center for Excellence in Nanoscience, Beijing Key Laboratory of Micro-Nano Energy and Sensor, Beijing Institute of Nanoenergy and Nanosystems, Chinese Academy of Sciences, 100083 Beijing, China.
- School of Nanoscience and Technology, University of Chinese Academy of Sciences, 100049 Beijing, China
| | - Zhong Lin Wang
- CAS Center for Excellence in Nanoscience, Beijing Key Laboratory of Micro-Nano Energy and Sensor, Beijing Institute of Nanoenergy and Nanosystems, Chinese Academy of Sciences, 100083 Beijing, China.
- School of Nanoscience and Technology, University of Chinese Academy of Sciences, 100049 Beijing, China
- School of Materials Science and Engineering, Georgia Institute of Technology, Atlanta, GA 30332-0245, USA
| |
Collapse
|
27
|
Barbieri L, Colin-York H, Korobchevskaya K, Li D, Wolfson DL, Karedla N, Schneider F, Ahluwalia BS, Seternes T, Dalmo RA, Dustin ML, Li D, Fritzsche M. Two-dimensional TIRF-SIM-traction force microscopy (2D TIRF-SIM-TFM). Nat Commun 2021; 12:2169. [PMID: 33846317 PMCID: PMC8041833 DOI: 10.1038/s41467-021-22377-9] [Citation(s) in RCA: 22] [Impact Index Per Article: 7.3] [Reference Citation Analysis] [Abstract] [Key Words] [MESH Headings] [Grants] [Track Full Text] [Download PDF] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Received: 06/01/2020] [Accepted: 03/12/2021] [Indexed: 02/01/2023] Open
Abstract
Quantifying small, rapidly evolving forces generated by cells is a major challenge for the understanding of biomechanics and mechanobiology in health and disease. Traction force microscopy remains one of the most broadly applied force probing technologies but typically restricts itself to slow events over seconds and micron-scale displacements. Here, we improve >2-fold spatially and >10-fold temporally the resolution of planar cellular force probing compared to its related conventional modalities by combining fast two-dimensional total internal reflection fluorescence super-resolution structured illumination microscopy and traction force microscopy. This live-cell 2D TIRF-SIM-TFM methodology offers a combination of spatio-temporal resolution enhancement relevant to forces on the nano- and sub-second scales, opening up new aspects of mechanobiology to analysis.
Collapse
Grants
- Biotechnology and Biological Sciences Research Council
- 212343/Z/18/Z Wellcome Trust
- 107457 Wellcome Trust
- 100262/Z/12/Z Wellcome Trust
- Wellcome Trust
- 091911 Wellcome Trust
- Medical Research Council
- L.B. would like to acknowledge funding from the Engineering and Physical Sciences Research Council (EPSRC) and Medical Research Council (EP/L016052/1). M.F., H.C.Y., K.K., and M.L.D. would like to thank the Rosalind Franklin Institute and the Kennedy Trust for Rheumatology Research (KTRR) for support. M.F., F.S., and H.C.Y. thank the Wellcome Trust (212343/Z/18/Z) and EPSRC (EP/S004459/1). M.L.D. also thank the Wellcome Trust for the Principal Research Fellowship awarded to M.D. (100262/Z/12/Z). Di.L. and D.L. are supported by a grant from the Chinese Ministry of Science and Technology (MOST: 2017YFA0505301, 2016YFA0500203), the National Natural Science Foundation of China (NSFC; 91754202, 31827802), and the Youth Innovation Promotion Association of Chinese Academy of Sciences (Grant No. 2020094). N.K. thanks the Alexander von Humboldt Foundation for funding his Feoder Lynen Fellowship. R.A.D acknowledge the Research Council of Norway (grant no. 301401) for funding. The TIRF-SIM platform was built in collaboration with and with funds from Micron (www.micronoxford.com), an Oxford-wide advanced microscopy technology consortium supported by Wellcome Strategic Awards (091911 and 107457) and an MRC/EPSRC/BBSRC next generation imaging award.
Collapse
Affiliation(s)
- Liliana Barbieri
- MRC Human Immunology Unit, Weatherall Institute of Molecular Medicine, University of Oxford, Oxford, UK
| | - Huw Colin-York
- MRC Human Immunology Unit, Weatherall Institute of Molecular Medicine, University of Oxford, Oxford, UK
- Kennedy Institute for Rheumatology, University of Oxford, Oxford, UK
| | | | - Di Li
- National Laboratory of Biomacromolecules, Institute of Biophysics, Chinese Academy of Sciences, Beijing, China
| | - Deanna L Wolfson
- Department of Physics and Technology, UiT The Arctic University of Norway, Tromsø, Norway
| | - Narain Karedla
- Kennedy Institute for Rheumatology, University of Oxford, Oxford, UK
- Rosalind Franklin Institute, Didcot, UK
| | - Falk Schneider
- MRC Human Immunology Unit, Weatherall Institute of Molecular Medicine, University of Oxford, Oxford, UK
- Kennedy Institute for Rheumatology, University of Oxford, Oxford, UK
| | - Balpreet S Ahluwalia
- Department of Physics and Technology, UiT The Arctic University of Norway, Tromsø, Norway
| | - Tore Seternes
- Norwegian College of Fishery Science, UiT The Arctic University of Norway, Tromsø, Norway
| | - Roy A Dalmo
- Norwegian College of Fishery Science, UiT The Arctic University of Norway, Tromsø, Norway
| | - Michael L Dustin
- Kennedy Institute for Rheumatology, University of Oxford, Oxford, UK
| | - Dong Li
- National Laboratory of Biomacromolecules, Institute of Biophysics, Chinese Academy of Sciences, Beijing, China.
- College of Life Sciences, University of Chinese Academy of Sciences, Beijing, China.
| | - Marco Fritzsche
- MRC Human Immunology Unit, Weatherall Institute of Molecular Medicine, University of Oxford, Oxford, UK.
- Kennedy Institute for Rheumatology, University of Oxford, Oxford, UK.
- Rosalind Franklin Institute, Didcot, UK.
| |
Collapse
|
28
|
Li D, Colin-York H, Barbieri L, Javanmardi Y, Guo Y, Korobchevskaya K, Moeendarbary E, Li D, Fritzsche M. Astigmatic traction force microscopy (aTFM). Nat Commun 2021; 12:2168. [PMID: 33846322 PMCID: PMC8042066 DOI: 10.1038/s41467-021-22376-w] [Citation(s) in RCA: 26] [Impact Index Per Article: 8.7] [Reference Citation Analysis] [Abstract] [Key Words] [MESH Headings] [Grants] [Track Full Text] [Download PDF] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Received: 06/01/2020] [Accepted: 03/12/2021] [Indexed: 01/23/2023] Open
Abstract
Quantifying small, rapidly progressing three-dimensional forces generated by cells remains a major challenge towards a more complete understanding of mechanobiology. Traction force microscopy is one of the most broadly applied force probing technologies but ascertaining three-dimensional information typically necessitates slow, multi-frame z-stack acquisition with limited sensitivity. Here, by performing traction force microscopy using fast single-frame astigmatic imaging coupled with total internal reflection fluorescence microscopy we improve the temporal resolution of three-dimensional mechanical force quantification up to 10-fold compared to its related super-resolution modalities. 2.5D astigmatic traction force microscopy (aTFM) thus enables live-cell force measurements approaching physiological sensitivity.
Collapse
Affiliation(s)
- Di Li
- National Laboratory of Biomacromolecules, CAS Center for Excellence in Biomacromolecules, Institute of Biophysics, Chinese Academy of Sciences, Beijing, China
| | - Huw Colin-York
- MRC Human Immunology Unit, Weatherall Institute of Molecular Medicine, University of Oxford, Oxford, UK
- Kennedy Institute for Rheumatology, University of Oxford, Oxford, UK
| | - Liliana Barbieri
- MRC Human Immunology Unit, Weatherall Institute of Molecular Medicine, University of Oxford, Oxford, UK
| | - Yousef Javanmardi
- Department of Mechanical Engineering, University College London, London, UK
| | - Yuting Guo
- National Laboratory of Biomacromolecules, CAS Center for Excellence in Biomacromolecules, Institute of Biophysics, Chinese Academy of Sciences, Beijing, China
| | | | - Emad Moeendarbary
- Department of Mechanical Engineering, University College London, London, UK.
| | - Dong Li
- National Laboratory of Biomacromolecules, CAS Center for Excellence in Biomacromolecules, Institute of Biophysics, Chinese Academy of Sciences, Beijing, China.
- College of Life Sciences, University of Chinese Academy of Sciences, Beijing, China.
| | - Marco Fritzsche
- MRC Human Immunology Unit, Weatherall Institute of Molecular Medicine, University of Oxford, Oxford, UK.
- Kennedy Institute for Rheumatology, University of Oxford, Oxford, UK.
- Rosalind Franklin Institute, Harwell Campus, Didcot, UK.
| |
Collapse
|
29
|
Zhang Z, Zheng T, Zhu R. Long-term and label-free monitoring for osteogenic differentiation of mesenchymal stem cells using force sensor and impedance measurement. J Mater Chem B 2020; 8:9913-9920. [PMID: 33034334 DOI: 10.1039/d0tb01968b] [Citation(s) in RCA: 4] [Impact Index Per Article: 1.0] [Reference Citation Analysis] [Abstract] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Indexed: 01/10/2023]
Abstract
Stem cells have attracted increasing research interest in the field of regenerative medicine due to their unique abilities to differentiate into multiple cell lineages. Label-free, real-time, and long-term monitoring for stem cell differentiation is requisite in studying directional differentiation and development mechanisms for tissue engineering applications, but a great challenge because of the rigorous demands for sensitivity, stability and biocompatibility of devices. In this article, a label-free and real-time monitoring approach using a zinc oxide (ZnO) nanorod field effect transistor (FET) is proposed to detect cell traction forces (CTFs) exerted by cells on underlying substrates. The ZnO nanorod FET with the approach of difference-frequency lock-in detection achieves high sensitivity, good stability, and excellent biocompatibility, by which real-time and long-term (over 20 days) monitoring of cellular mechanical changes in osteogenic differentiation of mesenchymal stem cells (MSCs) is successfully achieved. We also employ electrical impedance monitoring using microelectrode array chips and microscopic observation to investigate cell migration and nodular aggregation behaviors of MSCs in osteogenic differentiation. Various biochemical assays including alkaline phosphatase (ALP), osteopontin expression and alizarin red staining are utilized to verify osteogenic differentiation of MSCs. We propose a combination of cell traction force measurement, impedance measurement and microscopic observation to provide multimodal profiling of cell morphology, and cellular biomechanical and electrophysiological phenotypes, which can track cellular dynamics in stem cell development and help to deeply understand the mechanism of osteogenic differentiation.
Collapse
Affiliation(s)
- Zhizhong Zhang
- State Key Laboratory of Precision Measurement Technology and Instruments, Department of Precision Instrument, Tsinghua University, Beijing, 100084, China.
| | - Tianyang Zheng
- State Key Laboratory of Precision Measurement Technology and Instruments, Department of Precision Instrument, Tsinghua University, Beijing, 100084, China.
| | - Rong Zhu
- State Key Laboratory of Precision Measurement Technology and Instruments, Department of Precision Instrument, Tsinghua University, Beijing, 100084, China.
| |
Collapse
|
30
|
Epifluorescence-based three-dimensional traction force microscopy. Sci Rep 2020; 10:16599. [PMID: 33024138 PMCID: PMC7538907 DOI: 10.1038/s41598-020-72931-6] [Citation(s) in RCA: 11] [Impact Index Per Article: 2.8] [Reference Citation Analysis] [Abstract] [Track Full Text] [Download PDF] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Received: 05/29/2020] [Accepted: 09/04/2020] [Indexed: 02/02/2023] Open
Abstract
We introduce a novel method to compute three-dimensional (3D) displacements and both in-plane and out-of-plane tractions on nominally planar transparent materials using standard epifluorescence microscopy. Despite the importance of out-of-plane components to fully understanding cell behavior, epifluorescence images are generally not used for 3D traction force microscopy (TFM) experiments due to limitations in spatial resolution and measuring out-of-plane motion. To extend an epifluorescence-based technique to 3D, we employ a topology-based single particle tracking algorithm to reconstruct high spatial-frequency 3D motion fields from densely seeded single-particle layer images. Using an open-source finite element (FE) based solver, we then compute the 3D full-field stress and strain and surface traction fields. We demonstrate this technique by measuring tractions generated by both single human neutrophils and multicellular monolayers of Madin–Darby canine kidney cells, highlighting its acuity in reconstructing both individual and collective cellular tractions. In summary, this represents a new, easily accessible method for calculating fully three-dimensional displacement and 3D surface tractions at high spatial frequency from epifluorescence images. We released and support the complete technique as a free and open-source code package.
Collapse
|
31
|
Cellular census of human fibrosis defines functionally distinct stromal cell types and states. Nat Commun 2020; 11:2768. [PMID: 32488016 PMCID: PMC7265502 DOI: 10.1038/s41467-020-16264-y] [Citation(s) in RCA: 19] [Impact Index Per Article: 4.8] [Reference Citation Analysis] [Abstract] [Track Full Text] [Download PDF] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Received: 12/17/2019] [Accepted: 04/20/2020] [Indexed: 12/14/2022] Open
Abstract
Fibrotic disorders are some of the most devastating and poorly treated conditions in developed nations, yet effective therapeutics are not identified for many of them. A major barrier for the identification of targets and successful clinical translation is a limited understanding of the human fibrotic microenvironment. Here, we construct a stromal cell atlas of human fibrosis at single cell resolution from patients with Dupuytren’s disease, a localized fibrotic condition of the hand. A molecular taxonomy of the fibrotic milieu characterises functionally distinct stromal cell types and states, including a subset of immune regulatory ICAM1+ fibroblasts. In developing fibrosis, myofibroblasts exist along an activation continuum of phenotypically distinct populations. We also show that the tetraspanin CD82 regulates cell cycle progression and can be used as a cell surface marker of myofibroblasts. These findings have important implications for targeting core pathogenic drivers of human fibrosis. New anti-fibrotics aided by a better understanding of fibrotic cell subsets and their functions are needed. Here the authors perform single-cell RNA-seq and CyTOF on nodules from patients with Dupuytren’s disease to map subsets and the state of mesenchymal cells during pathogenic fibrogenesis.
Collapse
|
32
|
Rohena C, Kalogriopoulos N, Rajapakse N, Roy S, Lopez-Sanchez I, Ablack J, Sahoo D, Ghosh P. GIV•Kindlin Interaction Is Required for Kindlin-Mediated Integrin Recognition and Activation. iScience 2020; 23:101209. [PMID: 32535026 PMCID: PMC7300163 DOI: 10.1016/j.isci.2020.101209] [Citation(s) in RCA: 9] [Impact Index Per Article: 2.3] [Reference Citation Analysis] [Abstract] [Key Words] [Track Full Text] [Download PDF] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Received: 03/15/2020] [Revised: 04/15/2020] [Accepted: 05/24/2020] [Indexed: 11/16/2022] Open
Abstract
Cells perceive and respond to the extracellular matrix via integrin receptors; their dysregulation has been implicated in inflammation and cancer metastasis. Here we show that a guanine nucleotide-exchange modulator of trimeric-GTPase Gαi, GIV (a.k.a Girdin), directly binds the integrin adaptor Kindlin-2. A non-canonical short linear motif within the C terminus of GIV binds Kindlin-2-FERM3 domain at a site that is distinct from the binding site for the canonical NPxY motif on the -integrin tail. Binding of GIV to Kindlin-2 allosterically enhances Kindlin-2's affinity for β1-integrin. Consequently, integrin activation and clustering are maximized, which augments cell adhesion, spreading, and invasion. Findings elucidate how the GIV•Kindlin-2 complex has a 2-fold impact: it allosterically synergizes integrin activation and enables β1-integrins to indirectly access and modulate trimeric GTPases via the complex. Furthermore, Cox proportional-hazard models on tumor transcriptomics provide trans-scale evidence of synergistic interactions between GIV•Kindlin-2•β1-integrin on time to progression to metastasis. GIV and Kindlin (K2), two integrin adaptors that promote metastasis, bind each other Binding of GIV or integrin to K2 allosterically enhances GIV•K2•integrin complexes Binding is required for the maximal recruitment of GIV and K2 to active integrins Binding facilitates integrin clustering, activation, tumor cell adhesion, invasion
Collapse
Affiliation(s)
- Cristina Rohena
- Department of Medicine, University of California San Diego, 9500 Gilman Drive (MC 0651), George E. Palade Bldg, Rm 239, La Jolla, CA 92093, USA
| | - Nicholas Kalogriopoulos
- Department of Medicine, University of California San Diego, 9500 Gilman Drive (MC 0651), George E. Palade Bldg, Rm 239, La Jolla, CA 92093, USA; Department of Cellular and Molecular Medicine, University of California San Diego, CA 92093, USA
| | - Navin Rajapakse
- Department of Cellular and Molecular Medicine, University of California San Diego, CA 92093, USA
| | - Suchismita Roy
- Department of Cellular and Molecular Medicine, University of California San Diego, CA 92093, USA
| | - Inmaculada Lopez-Sanchez
- Department of Medicine, University of California San Diego, 9500 Gilman Drive (MC 0651), George E. Palade Bldg, Rm 239, La Jolla, CA 92093, USA
| | - Jailal Ablack
- Department of Medicine, University of California San Diego, 9500 Gilman Drive (MC 0651), George E. Palade Bldg, Rm 239, La Jolla, CA 92093, USA
| | - Debashis Sahoo
- Department of Pediatrics, University of California San Diego, CA 92093, USA; Department of Computer Science and Engineering, Jacob's School of Engineering, University of California San Diego, CA 92093, USA; Rebecca and John Moore Comprehensive Cancer Center, University of California San Diego, CA 92093, USA
| | - Pradipta Ghosh
- Department of Medicine, University of California San Diego, 9500 Gilman Drive (MC 0651), George E. Palade Bldg, Rm 239, La Jolla, CA 92093, USA; Department of Cellular and Molecular Medicine, University of California San Diego, CA 92093, USA; Rebecca and John Moore Comprehensive Cancer Center, University of California San Diego, CA 92093, USA; Veterans Affairs Medical Center, 3350 La Jolla Village Drive, San Diego, CA 92161, USA.
| |
Collapse
|
33
|
Layton TB, Williams L, Colin-York H, McCann FE, Cabrita M, Feldmann M, Brown C, Xie W, Fritzsche M, Furniss D, Nanchahal J. Single cell force profiling of human myofibroblasts reveals a biophysical spectrum of cell states. Biol Open 2020; 9:bio049809. [PMID: 32139395 PMCID: PMC7104857 DOI: 10.1242/bio.049809] [Citation(s) in RCA: 6] [Impact Index Per Article: 1.5] [Reference Citation Analysis] [Abstract] [Key Words] [MESH Headings] [Grants] [Track Full Text] [Download PDF] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Received: 12/02/2019] [Accepted: 02/21/2020] [Indexed: 01/31/2023] Open
Abstract
Mechanical force is a fundamental regulator of cell phenotype. Myofibroblasts are central mediators of fibrosis, a major unmet clinical need characterised by the deposition of excessive matrix proteins. Traction forces of myofibroblasts play a key role in remodelling the matrix and modulate the activities of embedded stromal cells. Here, we employ a combination of unsupervised computational analysis, cytoskeletal profiling and single cell traction force microscopy as a functional readout to uncover how the complex spatiotemporal dynamics and mechanics of living human myofibroblast shape sub-cellular profiling of traction forces in fibrosis. We resolve distinct biophysical communities of myofibroblasts, and our results provide a new paradigm for studying functional heterogeneity in human stromal cells.
Collapse
Affiliation(s)
- Thomas B Layton
- The Kennedy Institute of Rheumatology, Nuffield Department of Orthopaedics, Rheumatology and Musculoskeletal Sciences, University of Oxford, Oxford OX3 7FY, UK
| | - Lynn Williams
- The Kennedy Institute of Rheumatology, Nuffield Department of Orthopaedics, Rheumatology and Musculoskeletal Sciences, University of Oxford, Oxford OX3 7FY, UK
| | - Huw Colin-York
- MRC Human Immunology Unit, Weatherall Institute of Molecular Medicine, University of Oxford, Headley Way, Oxford OX3 9DS, UK
| | - Fiona E McCann
- The Kennedy Institute of Rheumatology, Nuffield Department of Orthopaedics, Rheumatology and Musculoskeletal Sciences, University of Oxford, Oxford OX3 7FY, UK
| | - Marisa Cabrita
- The Kennedy Institute of Rheumatology, Nuffield Department of Orthopaedics, Rheumatology and Musculoskeletal Sciences, University of Oxford, Oxford OX3 7FY, UK
| | - Marc Feldmann
- The Kennedy Institute of Rheumatology, Nuffield Department of Orthopaedics, Rheumatology and Musculoskeletal Sciences, University of Oxford, Oxford OX3 7FY, UK
| | - Cameron Brown
- Botnar Research Centre, Nuffield Department of Orthopaedics, Rheumatology and Musculoskeletal Sciences, University of Oxford, Oxford OX3 7LD, UK
| | - Weilin Xie
- Department of Inflammation Research, Celgene Corporation, San Diego, CA 92121, USA
| | - Marco Fritzsche
- The Kennedy Institute of Rheumatology, Nuffield Department of Orthopaedics, Rheumatology and Musculoskeletal Sciences, University of Oxford, Oxford OX3 7FY, UK
- MRC Human Immunology Unit, Weatherall Institute of Molecular Medicine, University of Oxford, Headley Way, Oxford OX3 9DS, UK
| | - Dominic Furniss
- Botnar Research Centre, Nuffield Department of Orthopaedics, Rheumatology and Musculoskeletal Sciences, University of Oxford, Oxford OX3 7LD, UK
| | - Jagdeep Nanchahal
- The Kennedy Institute of Rheumatology, Nuffield Department of Orthopaedics, Rheumatology and Musculoskeletal Sciences, University of Oxford, Oxford OX3 7FY, UK
| |
Collapse
|
34
|
Skamrahl M, Colin-York H, Barbieri L, Fritzsche M. Simultaneous Quantification of the Interplay Between Molecular Turnover and Cell Mechanics by AFM-FRAP. SMALL (WEINHEIM AN DER BERGSTRASSE, GERMANY) 2019; 15:e1902202. [PMID: 31419037 PMCID: PMC7612032 DOI: 10.1002/smll.201902202] [Citation(s) in RCA: 7] [Impact Index Per Article: 1.4] [Reference Citation Analysis] [Abstract] [Key Words] [MESH Headings] [Grants] [Track Full Text] [Subscribe] [Scholar Register] [Received: 05/01/2019] [Revised: 07/22/2019] [Indexed: 06/02/2023]
Abstract
Quantifying the adaptive mechanical behavior of living cells is essential for the understanding of their inner working and function. Yet, despite the establishment of quantitative methodologies correlating independent measurements of cell mechanics and its underlying molecular kinetics, explicit evidence and knowledge of the sensitivity of the feedback mechanisms of cells controlling their adaptive mechanics behavior remains elusive. Here, a combination of atomic force microscopy and fluorescence recovery after photobleaching is introduced offering simultaneous quantification and direct correlation of molecule kinetics and mechanics in living cells. Systematic application of this optomechanical atomic force microscopy-fluorescence recovery after photobleaching platform reveals changes in the actin turnover and filament lengths of ventral actin stress fibers in response to constant mechanical force at the apical actin cortex with a dynamic range from 0.1 to 10 nN, highlighting a direct relationship of active mechanosensation and adaptation of the cellular actin cytoskeleton. Simultaneous quantification of the relationship between molecule kinetics and cell mechanics may thus open-up unprecedented insights into adaptive mechanobiological mechanisms of cells.
Collapse
Affiliation(s)
- Mark Skamrahl
- MRC Human Immunology Unit, Weatherall Institute of Molecular Medicine, University of Oxford, Headley Way, Oxford. OX3 9DS, United Kingdom
| | - Huw Colin-York
- MRC Human Immunology Unit, Weatherall Institute of Molecular Medicine, University of Oxford, Headley Way, Oxford. OX3 9DS, United Kingdom
| | - Liliana Barbieri
- MRC Human Immunology Unit, Weatherall Institute of Molecular Medicine, University of Oxford, Headley Way, Oxford. OX3 9DS, United Kingdom
| | - Marco Fritzsche
- MRC Human Immunology Unit, Weatherall Institute of Molecular Medicine, University of Oxford, Headley Way, Oxford. OX3 9DS, United Kingdom
- Kennedy Institute for Rheumatology, Roosevelt Drive, University of Oxford, Oxford, OX3 7LF, United Kingdom
| |
Collapse
|
35
|
Abstract
In this study, economic magnetic tweezers (EMT) with a sharp gradient field were designed and built, in order to facilitate accurate force measurement. Our design costs less than 40 USD and is easy to mount onto most microscope stages. We leverage the computational fluidic dynamics techniques to calculate the forces based on the results obtained using our simple device. The EMT device is especially suitable to measure the traction forces at the dorsal side of a cell. As a proof of concept it was demonstrated that the EMT device could be applied to measure the dorsal traction forces exerted via the CD80-CTLA4 bond in metastatic cancer cells.
Collapse
|
36
|
Colin-York H, Javanmardi Y, Barbieri L, Li D, Korobchevskaya K, Guo Y, Hall C, Taylor A, Khuon S, Sheridan GK, Chew TL, Li D, Moeendarbary E, Fritzsche M. Spatiotemporally Super-Resolved Volumetric Traction Force Microscopy. NANO LETTERS 2019; 19:4427-4434. [PMID: 31199151 PMCID: PMC6628183 DOI: 10.1021/acs.nanolett.9b01196] [Citation(s) in RCA: 35] [Impact Index Per Article: 7.0] [Reference Citation Analysis] [Abstract] [Key Words] [MESH Headings] [Grants] [Track Full Text] [Subscribe] [Scholar Register] [Received: 03/22/2019] [Revised: 06/12/2019] [Indexed: 05/21/2023]
Abstract
Quantification of mechanical forces is a major challenge across biomedical sciences. Yet such measurements are essential to understanding the role of biomechanics in cell regulation and function. Traction force microscopy remains the most broadly applied force probing technology but typically restricts itself to single-plane two-dimensional quantifications with limited spatiotemporal resolution. Here, we introduce an enhanced force measurement technique combining 3D super-resolution fluorescence structural illumination microscopy and traction force microscopy (3D-SIM-TFM) offering increased spatiotemporal resolution, opening-up unprecedented insights into physiological three-dimensional force production in living cells.
Collapse
Affiliation(s)
- Huw Colin-York
- MRC
Human Immunology Unit, Weatherall Institute of Molecular Medicine, University of Oxford, Headley Way, Oxford OX3 9DS, United Kingdom
| | - Yousef Javanmardi
- Department
of Mechanical Engineering, University College
London, London WC1E 7JE, United Kingdom
| | - Liliana Barbieri
- MRC
Human Immunology Unit, Weatherall Institute of Molecular Medicine, University of Oxford, Headley Way, Oxford OX3 9DS, United Kingdom
| | - Di Li
- National
Laboratory of Biomacromolecules, Institute of Biophysics, Chinese Academy of Sciences, Beijing 100101, China
| | - Kseniya Korobchevskaya
- Kennedy
Institute for Rheumatology, University of
Oxford, Roosevelt Drive, Oxford OX3 7LF, United Kingdom
| | - Yuting Guo
- National
Laboratory of Biomacromolecules, Institute of Biophysics, Chinese Academy of Sciences, Beijing 100101, China
- College
of Life Sciences, University of Chinese
Academy of Sciences, Beijing 100049, China
| | - Chloe Hall
- Department
of Mechanical Engineering, University College
London, London WC1E 7JE, United Kingdom
| | - Aaron Taylor
- Howard Hughes
Medical Institute, Janelia Research Campus, 19700 Helix Drive, Ashburn, Virginia 20147, United States
| | - Satya Khuon
- Howard Hughes
Medical Institute, Janelia Research Campus, 19700 Helix Drive, Ashburn, Virginia 20147, United States
| | - Graham K. Sheridan
- School
of Pharmacy and Biomolecular Sciences, University
of Brighton, Brighton BN2 4AT, United Kingdom
| | - Teng-Leong Chew
- Howard Hughes
Medical Institute, Janelia Research Campus, 19700 Helix Drive, Ashburn, Virginia 20147, United States
| | - Dong Li
- National
Laboratory of Biomacromolecules, Institute of Biophysics, Chinese Academy of Sciences, Beijing 100101, China
- College
of Life Sciences, University of Chinese
Academy of Sciences, Beijing 100049, China
| | - Emad Moeendarbary
- Department
of Mechanical Engineering, University College
London, London WC1E 7JE, United Kingdom
- Department
of Biological Engineering, Massachusetts
Institute of Technology, Cambridge, Massachusetts 02139, United States
| | - Marco Fritzsche
- MRC
Human Immunology Unit, Weatherall Institute of Molecular Medicine, University of Oxford, Headley Way, Oxford OX3 9DS, United Kingdom
- Kennedy
Institute for Rheumatology, University of
Oxford, Roosevelt Drive, Oxford OX3 7LF, United Kingdom
| |
Collapse
|
37
|
Ungai-Salánki R, Peter B, Gerecsei T, Orgovan N, Horvath R, Szabó B. A practical review on the measurement tools for cellular adhesion force. Adv Colloid Interface Sci 2019; 269:309-333. [PMID: 31128462 DOI: 10.1016/j.cis.2019.05.005] [Citation(s) in RCA: 49] [Impact Index Per Article: 9.8] [Reference Citation Analysis] [Abstract] [Key Words] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Received: 02/22/2019] [Revised: 05/05/2019] [Accepted: 05/06/2019] [Indexed: 01/03/2023]
Abstract
Cell-cell and cell-matrix adhesions are fundamental in all multicellular organisms. They play a key role in cellular growth, differentiation, pattern formation and migration. Cell-cell adhesion is substantial in the immune response, pathogen-host interactions, and tumor development. The success of tissue engineering and stem cell implantations strongly depends on the fine control of live cell adhesion on the surface of natural or biomimetic scaffolds. Therefore, the quantitative and precise measurement of the adhesion strength of living cells is critical, not only in basic research but in modern technologies, too. Several techniques have been developed or are under development to quantify cell adhesion. All of them have their pros and cons, which has to be carefully considered before the experiments and interpretation of the recorded data. Current review provides a guide to choose the appropriate technique to answer a specific biological question or to complete a biomedical test by measuring cell adhesion.
Collapse
|
38
|
Colin-York H, Javanmardi Y, Skamrahl M, Kumari S, Chang VT, Khuon S, Taylor A, Chew TL, Betzig E, Moeendarbary E, Cerundolo V, Eggeling C, Fritzsche M. Cytoskeletal Control of Antigen-Dependent T Cell Activation. Cell Rep 2019; 26:3369-3379.e5. [PMID: 30893608 PMCID: PMC6426652 DOI: 10.1016/j.celrep.2019.02.074] [Citation(s) in RCA: 51] [Impact Index Per Article: 10.2] [Reference Citation Analysis] [Abstract] [Key Words] [MESH Headings] [Grants] [Track Full Text] [Download PDF] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Received: 12/11/2017] [Revised: 08/06/2018] [Accepted: 02/20/2019] [Indexed: 11/23/2022] Open
Abstract
Cytoskeletal actin dynamics is essential for T cell activation. Here, we show evidence that the binding kinetics of the antigen engaging the T cell receptor influences the nanoscale actin organization and mechanics of the immune synapse. Using an engineered T cell system expressing a specific T cell receptor and stimulated by a range of antigens, we found that the peak force experienced by the T cell receptor during activation was independent of the unbinding kinetics of the stimulating antigen. Conversely, quantification of the actin retrograde flow velocity at the synapse revealed a striking dependence on the antigen unbinding kinetics. These findings suggest that the dynamics of the actin cytoskeleton actively adjusted to normalize the force experienced by the T cell receptor in an antigen-specific manner. Consequently, tuning actin dynamics in response to antigen kinetics may thus be a mechanism that allows T cells to adjust the lengthscale and timescale of T cell receptor signaling.
Collapse
Affiliation(s)
- Huw Colin-York
- MRC Human Immunology Unit, Weatherall Institute of Molecular Medicine, University of Oxford, Headley Way, Oxford OX3 9DS, UK
| | - Yousef Javanmardi
- Department of Mechanical Engineering, University College London, London WC1E 7JE, UK
| | - Mark Skamrahl
- MRC Human Immunology Unit, Weatherall Institute of Molecular Medicine, University of Oxford, Headley Way, Oxford OX3 9DS, UK
| | - Sudha Kumari
- Koch Institute of Integrative Cancer Research, Massachusetts Institute of Technology, Cambridge, MA 02139, USA
| | - Veronica T Chang
- MRC Laboratory of Molecular Biology, Francis Crick Avenue, Cambridge Biomedical Campus, Cambridge CB2 0QH, UK
| | - Satya Khuon
- Janelia Research Campus, Howard Hughes Medical Institute, 19700 Helix Drive, Ashburn, VA 20147, USA
| | - Aaron Taylor
- Janelia Research Campus, Howard Hughes Medical Institute, 19700 Helix Drive, Ashburn, VA 20147, USA
| | - Teng-Leong Chew
- Janelia Research Campus, Howard Hughes Medical Institute, 19700 Helix Drive, Ashburn, VA 20147, USA
| | - Eric Betzig
- Janelia Research Campus, Howard Hughes Medical Institute, 19700 Helix Drive, Ashburn, VA 20147, USA
| | - Emad Moeendarbary
- Department of Mechanical Engineering, University College London, London WC1E 7JE, UK; Department of Biological Engineering, Massachusetts Institute of Technology, Cambridge, MA 02139, USA
| | - Vincenzo Cerundolo
- MRC Human Immunology Unit, Weatherall Institute of Molecular Medicine, University of Oxford, Headley Way, Oxford OX3 9DS, UK
| | - Christian Eggeling
- MRC Human Immunology Unit, Weatherall Institute of Molecular Medicine, University of Oxford, Headley Way, Oxford OX3 9DS, UK
| | - Marco Fritzsche
- MRC Human Immunology Unit, Weatherall Institute of Molecular Medicine, University of Oxford, Headley Way, Oxford OX3 9DS, UK; Kennedy Institute for Rheumatology, University of Oxford, Roosevelt Drive, Oxford OX3 7LF, UK.
| |
Collapse
|
39
|
Mulligan JA, Feng X, Adie SG. Quantitative reconstruction of time-varying 3D cell forces with traction force optical coherence microscopy. Sci Rep 2019; 9:4086. [PMID: 30858424 PMCID: PMC6411852 DOI: 10.1038/s41598-019-40608-4] [Citation(s) in RCA: 26] [Impact Index Per Article: 5.2] [Reference Citation Analysis] [Abstract] [MESH Headings] [Grants] [Track Full Text] [Download PDF] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Received: 10/16/2018] [Accepted: 02/19/2019] [Indexed: 12/18/2022] Open
Abstract
Cellular traction forces (CTFs) play an integral role in both physiological processes and disease, and are a topic of interest in mechanobiology. Traction force microscopy (TFM) is a family of methods used to quantify CTFs in a variety of settings. State-of-the-art 3D TFM methods typically rely on confocal fluorescence microscopy, which can impose limitations on acquisition speed, volumetric coverage, and temporal sampling or coverage. In this report, we present the first quantitative implementation of a new TFM technique: traction force optical coherence microscopy (TF-OCM). TF-OCM leverages the capabilities of optical coherence microscopy and computational adaptive optics (CAO) to enable the quantitative reconstruction of 3D CTFs in scattering media with minute-scale temporal sampling. We applied TF-OCM to quantify CTFs exerted by isolated NIH-3T3 fibroblasts embedded in Matrigel, with five-minute temporal sampling, using images spanning a 500 × 500 × 500 μm3 field-of-view. Due to the reliance of TF-OCM on computational imaging methods, we have provided extensive discussion of the equations, assumptions, and failure modes of these methods. By providing high-throughput, label-free, volumetric imaging in scattering media, TF-OCM is well-suited to the study of 3D CTF dynamics, and may prove advantageous for the study of large cell collectives, such as the spheroid models prevalent in mechanobiology.
Collapse
Affiliation(s)
- Jeffrey A Mulligan
- School of Electrical and Computer Engineering, Cornell University, Ithaca, New York, 14853, USA
| | - Xinzeng Feng
- Institute for Computational Engineering and Sciences, The University of Texas at Austin, Austin, Texas, 78712, USA
| | - Steven G Adie
- Nancy E. and Peter C. Meinig School of Biomedical Engineering, Cornell University, Ithaca, New York, 14853, USA.
| |
Collapse
|
40
|
Colin-York H, Li D, Korobchevskaya K, Chang VT, Betzig E, Eggeling C, Fritzsche M. Cytoskeletal actin patterns shape mast cell activation. Commun Biol 2019; 2:93. [PMID: 30854485 PMCID: PMC6405992 DOI: 10.1038/s42003-019-0322-9] [Citation(s) in RCA: 26] [Impact Index Per Article: 5.2] [Reference Citation Analysis] [Abstract] [Download PDF] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Received: 10/31/2018] [Accepted: 01/22/2019] [Indexed: 01/05/2023] Open
Abstract
Activation of immune cells relies on a dynamic actin cytoskeleton. Despite detailed knowledge of molecular actin assembly, the exact processes governing actin organization during activation remain elusive. Using advanced microscopy, we here show that Rat Basophilic Leukemia (RBL) cells, a model mast cell line, employ an orchestrated series of reorganization events within the cortical actin network during activation. In response to IgE antigen-stimulation of FCε receptors (FCεR) at the RBL cell surface, we observed symmetry breaking of the F-actin network and subsequent rapid disassembly of the actin cortex. This was followed by a reassembly process that may be driven by the coordinated transformation of distinct nanoscale F-actin architectures, reminiscent of self-organizing actin patterns. Actin patterns co-localized with zones of Arp2/3 nucleation, while network reassembly was accompanied by myosin-II activity. Strikingly, cortical actin disassembly coincided with zones of granule secretion, suggesting that cytoskeletal actin patterns contribute to orchestrate RBL cell activation. Huw Colin-York et al. use advanced microscopy techniques to show that the cortical actin network within a model mast cell line undergoes a series of reorganizational events at the basal interface during activation. They find that actin patterns co-localize with zones of Arp2/3 nucleation and myosin-II activity accompanies network reassembly.
Collapse
Affiliation(s)
- Huw Colin-York
- MRC Human Immunology Unit, Weatherall Institute of Molecular Medicine, University of Oxford, Headley Way, Oxford, OX3 9DS, UK
| | - Dong Li
- Howard Hughes Medical Institute, Janelia Research Campus, 19700 Helix Drive, Ashburn, VA, 20147, USA.,National Laboratory of Biomacromolecules, Institute of Biophysics, Chinese Academy of Sciences, Beijing, 100101, China
| | - Kseniya Korobchevskaya
- Kennedy Institute for Rheumatology, University of Oxford, Roosevelt Drive, Oxford, OX3 7LF, UK
| | - Veronica T Chang
- MRC Laboratory of Molecular Biology, University of Cambridge, Cambridge, CB2 0QH, UK
| | - Eric Betzig
- Howard Hughes Medical Institute, Janelia Research Campus, 19700 Helix Drive, Ashburn, VA, 20147, USA
| | - Christian Eggeling
- MRC Human Immunology Unit, Weatherall Institute of Molecular Medicine, University of Oxford, Headley Way, Oxford, OX3 9DS, UK
| | - Marco Fritzsche
- MRC Human Immunology Unit, Weatherall Institute of Molecular Medicine, University of Oxford, Headley Way, Oxford, OX3 9DS, UK. .,Kennedy Institute for Rheumatology, University of Oxford, Roosevelt Drive, Oxford, OX3 7LF, UK.
| |
Collapse
|
41
|
Callaghan NI, Hadipour-Lakmehsari S, Lee SH, Gramolini AO, Simmons CA. Modeling cardiac complexity: Advancements in myocardial models and analytical techniques for physiological investigation and therapeutic development in vitro. APL Bioeng 2019; 3:011501. [PMID: 31069331 PMCID: PMC6481739 DOI: 10.1063/1.5055873] [Citation(s) in RCA: 9] [Impact Index Per Article: 1.8] [Reference Citation Analysis] [Abstract] [Track Full Text] [Download PDF] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Received: 09/11/2018] [Accepted: 12/31/2018] [Indexed: 02/06/2023] Open
Abstract
Cardiomyopathies, heart failure, and arrhythmias or conduction blockages impact millions of patients worldwide and are associated with marked increases in sudden cardiac death, decline in the quality of life, and the induction of secondary pathologies. These pathologies stem from dysfunction in the contractile or conductive properties of the cardiomyocyte, which as a result is a focus of fundamental investigation, drug discovery and therapeutic development, and tissue engineering. All of these foci require in vitro myocardial models and experimental techniques to probe the physiological functions of the cardiomyocyte. In this review, we provide a detailed exploration of different cell models, disease modeling strategies, and tissue constructs used from basic to translational research. Furthermore, we highlight recent advancements in imaging, electrophysiology, metabolic measurements, and mechanical and contractile characterization modalities that are advancing our understanding of cardiomyocyte physiology. With this review, we aim to both provide a biological framework for engineers contributing to the field and demonstrate the technical basis and limitations underlying physiological measurement modalities for biologists attempting to take advantage of these state-of-the-art techniques.
Collapse
Affiliation(s)
| | | | | | | | - Craig A. Simmons
- Author to whom correspondence should be addressed: . Present address: Ted Rogers Centre for Heart
Research, 661 University Avenue, 14th Floor Toronto, Ontario M5G 1M1, Canada. Tel.:
416-946-0548. Fax: 416-978-7753
| |
Collapse
|
42
|
Dannert C, Stokke BT, Dias RS. Nanoparticle-Hydrogel Composites: From Molecular Interactions to Macroscopic Behavior. Polymers (Basel) 2019; 11:E275. [PMID: 30960260 PMCID: PMC6419045 DOI: 10.3390/polym11020275] [Citation(s) in RCA: 99] [Impact Index Per Article: 19.8] [Reference Citation Analysis] [Abstract] [Key Words] [Track Full Text] [Download PDF] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Received: 11/22/2018] [Revised: 01/23/2019] [Accepted: 01/27/2019] [Indexed: 12/21/2022] Open
Abstract
Hydrogels are materials used in a variety of applications, ranging from tissue engineering to drug delivery. The incorporation of nanoparticles to yield composite hydrogels has gained substantial momentum over the years since these afford tailor-making and extend material mechanical properties far beyond those achievable through molecular design of the network component. Here, we review different procedures that have been used to integrate nanoparticles into hydrogels; the types of interactions acting between polymers and nanoparticles; and how these underpin the improved mechanical and optical properties of the gels, including the self-healing ability of these composite gels, as well as serving as the basis for future development. In a less explored approach, hydrogels have been used as dispersants of nanomaterials, allowing a larger exposure of the surface of the nanomaterial and thus a better performance in catalytic and sensor applications. Furthermore, the reporting capacity of integrated nanoparticles in hydrogels to assess hydrogel properties, such as equilibrium swelling and elasticity, is highlighted.
Collapse
Affiliation(s)
- Corinna Dannert
- Department of Physics, NTNU- Norwegian University of Science and Technology, NO-7491 Trondheim, Norway.
| | - Bjørn Torger Stokke
- Department of Physics, NTNU- Norwegian University of Science and Technology, NO-7491 Trondheim, Norway.
| | - Rita S Dias
- Department of Physics, NTNU- Norwegian University of Science and Technology, NO-7491 Trondheim, Norway.
| |
Collapse
|
43
|
Matellan C, Del Río Hernández AE. Where No Hand Has Gone Before: Probing Mechanobiology at the Cellular Level. ACS Biomater Sci Eng 2018; 5:3703-3719. [PMID: 33405886 DOI: 10.1021/acsbiomaterials.8b01206] [Citation(s) in RCA: 16] [Impact Index Per Article: 2.7] [Reference Citation Analysis] [Abstract] [Key Words] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Indexed: 01/05/2023]
Abstract
Physical forces and other mechanical stimuli are fundamental regulators of cell behavior and function. Cells are also biomechanically competent: they generate forces to migrate, contract, remodel, and sense their environment. As the knowledge of the mechanisms of mechanobiology increases, the need to resolve and probe increasingly small scales calls for novel technologies to mechanically manipulate cells, examine forces exerted by cells, and characterize cellular biomechanics. Here, we review novel methods to quantify cellular force generation, measure cell mechanical properties, and exert localized piconewton and nanonewton forces on cells, receptors, and proteins. The combination of these technologies will provide further insight on the effect of mechanical stimuli on cells and the mechanisms that convert these stimuli into biochemical and biomechanical activity.
Collapse
Affiliation(s)
- Carlos Matellan
- Cellular and Molecular Biomechanics Laboratory, Department of Bioengineering, Imperial College London, London SW7 2AZ, United Kingdom
| | - Armando E Del Río Hernández
- Cellular and Molecular Biomechanics Laboratory, Department of Bioengineering, Imperial College London, London SW7 2AZ, United Kingdom
| |
Collapse
|
44
|
Ando T, Bhamidimarri SP, Brending N, Colin-York H, Collinson L, De Jonge N, de Pablo PJ, Debroye E, Eggeling C, Franck C, Fritzsche M, Gerritsen H, Giepmans BNG, Grunewald K, Hofkens J, Hoogenboom JP, Janssen KPF, Kaufman R, Klumpermann J, Kurniawan N, Kusch J, Liv N, Parekh V, Peckys DB, Rehfeldt F, Reutens DC, Roeffaers MBJ, Salditt T, Schaap IAT, Schwarz US, Verkade P, Vogel MW, Wagner R, Winterhalter M, Yuan H, Zifarelli G. The 2018 correlative microscopy techniques roadmap. JOURNAL OF PHYSICS D: APPLIED PHYSICS 2018; 51:443001. [PMID: 30799880 PMCID: PMC6372154 DOI: 10.1088/1361-6463/aad055] [Citation(s) in RCA: 79] [Impact Index Per Article: 13.2] [Reference Citation Analysis] [Abstract] [Key Words] [Grants] [Track Full Text] [Subscribe] [Scholar Register] [Received: 02/09/2018] [Revised: 06/14/2018] [Accepted: 07/01/2018] [Indexed: 05/19/2023]
Abstract
Developments in microscopy have been instrumental to progress in the life sciences, and many new techniques have been introduced and led to new discoveries throughout the last century. A wide and diverse range of methodologies is now available, including electron microscopy, atomic force microscopy, magnetic resonance imaging, small-angle x-ray scattering and multiple super-resolution fluorescence techniques, and each of these methods provides valuable read-outs to meet the demands set by the samples under study. Yet, the investigation of cell development requires a multi-parametric approach to address both the structure and spatio-temporal organization of organelles, and also the transduction of chemical signals and forces involved in cell-cell interactions. Although the microscopy technologies for observing each of these characteristics are well developed, none of them can offer read-out of all characteristics simultaneously, which limits the information content of a measurement. For example, while electron microscopy is able to disclose the structural layout of cells and the macromolecular arrangement of proteins, it cannot directly follow dynamics in living cells. The latter can be achieved with fluorescence microscopy which, however, requires labelling and lacks spatial resolution. A remedy is to combine and correlate different readouts from the same specimen, which opens new avenues to understand structure-function relations in biomedical research. At the same time, such correlative approaches pose new challenges concerning sample preparation, instrument stability, region of interest retrieval, and data analysis. Because the field of correlative microscopy is relatively young, the capabilities of the various approaches have yet to be fully explored, and uncertainties remain when considering the best choice of strategy and workflow for the correlative experiment. With this in mind, the Journal of Physics D: Applied Physics presents a special roadmap on the correlative microscopy techniques, giving a comprehensive overview from various leading scientists in this field, via a collection of multiple short viewpoints.
Collapse
Affiliation(s)
- Toshio Ando
- Nano Life Science Institute (WPI-NanoLSI), Kanazawa University, Kanazawa, Japan
| | | | | | - H Colin-York
- MRC Human Immunology Unit, Weatherall Institute of Molecular Medicine, University of Oxford, Headley Way, OX3 9DS Oxford, United Kingdom
| | | | - Niels De Jonge
- INM-Leibniz Institute for New Materials, 66123 Saarbrücken, Germany
- Saarland University, 66123 Saarbrücken, Germany
| | - P J de Pablo
- Dpto. Física de la Materia Condensada Universidad Autónoma de Madrid 28049, Madrid, Spain
- Instituto de Física de la Materia Condensada IFIMAC, Universidad Autónoma de Madrid 28049, Madrid, Spain
| | - Elke Debroye
- KU Leuven, Department of Chemistry, B-3001 Heverlee, Belgium
| | - Christian Eggeling
- MRC Human Immunology Unit, Weatherall Institute of Molecular Medicine, University of Oxford, Headley Way, OX3 9DS Oxford, United Kingdom
- Institute of Applied Optics, Friedrich-Schiller University, Jena, Germany
- Leibniz Institute of Photonic Technology (IPHT), Jena, Germany
| | - Christian Franck
- Department of Mechanical Engineering, University of Wisconsin-Madison, 1513 University Ave, Madison, WI 53706, United States of America
| | - Marco Fritzsche
- MRC Human Immunology Unit, Weatherall Institute of Molecular Medicine, University of Oxford, Headley Way, OX3 9DS Oxford, United Kingdom
- Kennedy Institute for Rheumatology, University of Oxford, Oxford, United Kingdom
| | - Hans Gerritsen
- Debye Institute, Utrecht University, Utrecht, Netherlands
| | - Ben N G Giepmans
- Department of Cell Biology, University of Groningen, University Medical Center Groningen, Groningen, Netherlands
| | - Kay Grunewald
- Division of Structural Biology, Wellcome Trust Centre for Human Genetics, University of Oxford, Oxford, United Kingdom
- Centre of Structural Systems Biology Hamburg and University of Hamburg, Hamburg, Germany
- Heinrich-Pette-Institute, Leibniz Institute of Virology, Hamburg, Germany
| | - Johan Hofkens
- KU Leuven, Department of Chemistry, B-3001 Heverlee, Belgium
| | | | | | - Rainer Kaufman
- Division of Structural Biology, Wellcome Trust Centre for Human Genetics, University of Oxford, Oxford, United Kingdom
- Centre of Structural Systems Biology Hamburg and University of Hamburg, Hamburg, Germany
- Department of Biochemistry, University of Oxford, Oxford, United Kingdom
| | - Judith Klumpermann
- Section Cell Biology, Center for Molecular Medicine, University Medical Center Utrecht, Utrecht University, Heidelberglaan 100, 3584CX Utrecht, Netherlands
| | - Nyoman Kurniawan
- Centre for Advanced Imaging, The University of Queensland, Brisbane, QLD 4072, Australia
| | | | - Nalan Liv
- Section Cell Biology, Center for Molecular Medicine, University Medical Center Utrecht, Utrecht University, Heidelberglaan 100, 3584CX Utrecht, Netherlands
| | - Viha Parekh
- Centre for Advanced Imaging, The University of Queensland, Brisbane, QLD 4072, Australia
| | - Diana B Peckys
- Faculty of Medicine, Saarland University, 66421 Homburg, Germany
| | - Florian Rehfeldt
- University of Göttingen, Third Institute of Physics-Biophysics, 37077 Göttingen, Germany
| | - David C Reutens
- Centre for Advanced Imaging, The University of Queensland, Brisbane, QLD 4072, Australia
| | | | - Tim Salditt
- University of Göttingen, Institute for X-Ray Physics, 37077 Göttingen, Germany
| | - Iwan A T Schaap
- SmarAct GmbH, Schütte-Lanz-Str. 9, D-26135 Oldenburg, Germany
| | - Ulrich S Schwarz
- Institute for Theoretical Physics and BioQuant, Heidelberg University, Heidelberg, Germany
| | - Paul Verkade
- School of Biochemistry, University of Bristol, Bristol, United Kingdom
| | - Michael W Vogel
- Centre for Advanced Imaging, The University of Queensland, Brisbane, QLD 4072, Australia
| | - Richard Wagner
- Department of Life Sciences & Chemistry, Jacobs University, Bremen, Germany
| | | | - Haifeng Yuan
- KU Leuven, Department of Chemistry, B-3001 Heverlee, Belgium
| | - Giovanni Zifarelli
- Department of Physiology, Anatomy and Genetics, University of Oxford, Oxford, United Kingdom
| |
Collapse
|
45
|
Maskless Surface Modification of Polyurethane Films by an Atmospheric Pressure He/O₂ Plasma Microjet for Gelatin Immobilization. MICROMACHINES 2018; 9:mi9040195. [PMID: 30424128 PMCID: PMC6187667 DOI: 10.3390/mi9040195] [Citation(s) in RCA: 6] [Impact Index Per Article: 1.0] [Reference Citation Analysis] [Abstract] [Key Words] [Track Full Text] [Download PDF] [Figures] [Subscribe] [Scholar Register] [Received: 02/01/2018] [Revised: 04/01/2018] [Accepted: 04/17/2018] [Indexed: 01/28/2023]
Abstract
A localized maskless modification method of polyurethane (PU) films through an atmospheric pressure He/O2 plasma microjet (APPμJ) was proposed. The APPμJ system combines an atmospheric pressure plasma jet (APPJ) with a microfabricated silicon micronozzle with dimension of 30 μm, which has advantages of simple structure and low cost. The possibility of APPμJ in functionalizing PU films with hydroxyl (–OH) groups and covalent grafting of gelatin for improving its biocompatibility was demonstrated. The morphologies and chemical compositions of the modified surface were analyzed by scanning electronic microscopy (SEM), Raman spectroscopy, and X-ray photoelectron spectroscopy (XPS). The fluorescent images show the modified surface can be divided into four areas with different fluorescence intensity from the center to the outside domain. The distribution of the rings could be controlled by plasma process parameters, such as the treatment time and the flow rate of O2. When the treatment time is 4 to 5 min with the oxygen percentage of 0.6%, the PU film can be effectively local functionalized with the diameter of 170 μm. In addition, the modification mechanism of PU films by the APPμJ is investigated. The localized polymer modified by APPμJ has potential applications in the field of tissue engineering.
Collapse
|
46
|
Rajagopal V, Holmes WR, Lee PVS. Computational modeling of single-cell mechanics and cytoskeletal mechanobiology. WILEY INTERDISCIPLINARY REVIEWS. SYSTEMS BIOLOGY AND MEDICINE 2018; 10:e1407. [PMID: 29195023 PMCID: PMC5836888 DOI: 10.1002/wsbm.1407] [Citation(s) in RCA: 31] [Impact Index Per Article: 5.2] [Reference Citation Analysis] [Abstract] [MESH Headings] [Track Full Text] [Download PDF] [Figures] [Subscribe] [Scholar Register] [Received: 04/07/2017] [Revised: 08/19/2017] [Accepted: 09/07/2017] [Indexed: 01/10/2023]
Abstract
Cellular cytoskeletal mechanics plays a major role in many aspects of human health from organ development to wound healing, tissue homeostasis and cancer metastasis. We summarize the state-of-the-art techniques for mathematically modeling cellular stiffness and mechanics and the cytoskeletal components and factors that regulate them. We highlight key experiments that have assisted model parameterization and compare the advantages of different models that have been used to recapitulate these experiments. An overview of feed-forward mechanisms from signaling to cytoskeleton remodeling is provided, followed by a discussion of the rapidly growing niche of encapsulating feedback mechanisms from cytoskeletal and cell mechanics to signaling. We discuss broad areas of advancement that could accelerate research and understanding of cellular mechanobiology. A precise understanding of the molecular mechanisms that affect cell and tissue mechanics and function will underpin innovations in medical device technologies of the future. WIREs Syst Biol Med 2018, 10:e1407. doi: 10.1002/wsbm.1407 This article is categorized under: Models of Systems Properties and Processes > Mechanistic Models Physiology > Mammalian Physiology in Health and Disease Models of Systems Properties and Processes > Cellular Models.
Collapse
Affiliation(s)
- Vijay Rajagopal
- Cell Structure and Mechanobiology Group, Department of Biomedical EngineeringUniversity of MelbourneMelbourneAustralia
| | - William R. Holmes
- Department of Physics and AstronomyVanderbilt UniversityNashvilleTNUSA
| | - Peter Vee Sin Lee
- Cell and Tissue Biomechanics Laboratory, Department of Biomedical EngineeringUniversity of MelbourneMelbourneAustralia
| |
Collapse
|
47
|
|
48
|
Mulligan JA, Bordeleau F, Reinhart-King CA, Adie SG. Traction Force Microscopy for Noninvasive Imaging of Cell Forces. ADVANCES IN EXPERIMENTAL MEDICINE AND BIOLOGY 2018; 1092:319-349. [PMID: 30368759 DOI: 10.1007/978-3-319-95294-9_15] [Citation(s) in RCA: 14] [Impact Index Per Article: 2.3] [Reference Citation Analysis] [Abstract] [Key Words] [MESH Headings] [Grants] [Track Full Text] [Subscribe] [Scholar Register] [Indexed: 12/25/2022]
Abstract
The forces exerted by cells on their surroundings play an integral role in both physiological processes and disease progression. Traction force microscopy is a noninvasive technique that enables the in vitro imaging and quantification of cell forces. Utilizing expertise from a variety of disciplines, recent developments in traction force microscopy are enhancing the study of cell forces in physiologically relevant model systems, and hold promise for further advancing knowledge in mechanobiology. In this chapter, we discuss the methods, capabilities, and limitations of modern approaches for traction force microscopy, and highlight ongoing efforts and challenges underlying future innovations.
Collapse
Affiliation(s)
- Jeffrey A Mulligan
- School of Electrical and Computer Engineering, Cornell University, Ithaca, NY, USA
| | - François Bordeleau
- Centre de Recherche du CHU de Québec, Université Laval, Québec, Qc, Canada
- Départment of Biologie Moléculaire, Biochimie Médicale et Pathologie, Université Laval, Québec, Qc, Canada
| | - Cynthia A Reinhart-King
- Department of Biomedical Engineering, Vanderbilt University, Nashville, TN, USA
- Meinig School of Biomedical Engineering, Cornell University, Ithaca, NY, USA
| | - Steven G Adie
- Meinig School of Biomedical Engineering, Cornell University, Ithaca, NY, USA.
| |
Collapse
|
49
|
Chang JC, Liu Y, Chou T. Reconstruction of Cell Focal Adhesions using Physical Constraints and Compressive Regularization. Biophys J 2017; 113:2530-2539. [PMID: 29212006 PMCID: PMC5738527 DOI: 10.1016/j.bpj.2017.09.021] [Citation(s) in RCA: 1] [Impact Index Per Article: 0.1] [Reference Citation Analysis] [Abstract] [MESH Headings] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Received: 06/27/2017] [Revised: 09/13/2017] [Accepted: 09/19/2017] [Indexed: 11/30/2022] Open
Abstract
We develop a method to reconstruct, from measured displacements of an underlying elastic substrate, the spatially dependent forces that cells or tissues impart on it. Given newly available high-resolution images of substrate displacements, it is desirable to be able to reconstruct small-scale, compactly supported focal adhesions that are often localized and exist only within the footprint of a cell. In addition to the standard quadratic data mismatch terms that define least-squares fitting, we motivate a regularization term in the objective function that penalizes vectorial invariants of the reconstructed surface stress while preserving boundaries. We solve this inverse problem by providing a numerical method for setting up a discretized inverse problem that is solvable by standard convex optimization techniques. By minimizing the objective function subject to a number of important physically motivated constraints, we are able to efficiently reconstruct stress fields with localized structure from simulated and experimental substrate displacements. Our method incorporates the exact solution for a stress tensor accurate to first-order finite differences and motivates the use of distance-based cutoffs for data inclusion and problem sparsification.
Collapse
Affiliation(s)
- Joshua C Chang
- Epidemiology and Biostatistics Section, Rehabilitation Medicine, Clinical Center, The National Institutes of Health, Bethesda, Maryland
| | - Yanli Liu
- Department of Mathematics, UCLA, Los Angeles, California
| | - Tom Chou
- Department of Mathematics, UCLA, Los Angeles, California; Department of Biomathematics, UCLA, Los Angeles, California.
| |
Collapse
|
50
|
Sun Y, Deng R, Zhang K, Ren X, Zhang L, Li J. Single-cell study of the extracellular matrix effect on cell growth by in situ imaging of gene expression. Chem Sci 2017; 8:8019-8024. [PMID: 29568449 PMCID: PMC5855132 DOI: 10.1039/c7sc03880a] [Citation(s) in RCA: 15] [Impact Index Per Article: 2.1] [Reference Citation Analysis] [Abstract] [Track Full Text] [Download PDF] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Received: 09/05/2017] [Accepted: 10/01/2017] [Indexed: 12/16/2022] Open
Abstract
The effect of extracellular matrix stiffness on cell growth and the underlying molecular mechanism was investigated using an in situ single-cell imaging of gene expression method based on rolling circle amplification.
Cell behaviors are known to be regulated by the cellular microenvironment. Traditional cell-population based analysis methods need to separate cells from their extracellular matrix (ECM) and cannot resolve the heterogeneity of cell behaviors. Herein, an in situ single-cell analysis method based on rolling circle amplification was exploited to image gene expression in single cells for investigating the effect of ECM stiffness on cell growth. This method enables the simultaneous quantifying of the cell phenotype and gene expression at the single-cell level, which can help in understanding the underlying molecular mechanism of cell growth. It is found that ECM stiffness could affect cell growth via regulating the expression level of the cytoskeleton-assembly associated genes PFN1 and CFL1 and their co-expression pattern. Therefore, this single-cell analysis platform may facilitate us to tap into the study of “single-cell phenotypes” and elucidate the disease association of ECMs.
Collapse
Affiliation(s)
- Yupeng Sun
- Department of Chemistry , Key Laboratory of Bioorganic Phosphorus Chemistry & Chemical Biology , Tsinghua University , Beijing 100084 , China .
| | - Ruijie Deng
- Department of Chemistry , Key Laboratory of Bioorganic Phosphorus Chemistry & Chemical Biology , Tsinghua University , Beijing 100084 , China .
| | - Kaixiang Zhang
- Department of Chemistry , Key Laboratory of Bioorganic Phosphorus Chemistry & Chemical Biology , Tsinghua University , Beijing 100084 , China .
| | - Xiaojun Ren
- Department of Chemistry , Key Laboratory of Bioorganic Phosphorus Chemistry & Chemical Biology , Tsinghua University , Beijing 100084 , China .
| | - Ling Zhang
- Department of Chemistry , Key Laboratory of Bioorganic Phosphorus Chemistry & Chemical Biology , Tsinghua University , Beijing 100084 , China .
| | - Jinghong Li
- Department of Chemistry , Key Laboratory of Bioorganic Phosphorus Chemistry & Chemical Biology , Tsinghua University , Beijing 100084 , China .
| |
Collapse
|