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Lipp SN, Jacobson KR, Colling HA, Tuttle TG, Miles DT, McCreery KP, Calve S. Mechanical loading is required for initiation of extracellular matrix deposition at the developing murine myotendinous junction. Matrix Biol 2023; 116:28-48. [PMID: 36709857 PMCID: PMC10218368 DOI: 10.1016/j.matbio.2023.01.003] [Citation(s) in RCA: 4] [Impact Index Per Article: 4.0] [Reference Citation Analysis] [Abstract] [Key Words] [MESH Headings] [Grants] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Received: 06/26/2022] [Revised: 01/17/2023] [Accepted: 01/24/2023] [Indexed: 01/27/2023]
Abstract
The myotendinous junction (MTJ) contributes to the generation of motion by connecting muscle to tendon. At the adult MTJ, a specialized extracellular matrix (ECM) is thought to contribute to the mechanical integrity of the muscle-tendon interface, but the factors that influence MTJ formation during mammalian development are unclear. Here, we combined 3D imaging and proteomics with murine models in which muscle contractility and patterning are disrupted to resolve morphological and compositional changes in the ECM during MTJ development. We found that MTJ-specific ECM deposition can be initiated via static loading due to growth; however, it required cyclic loading to develop a mature morphology. Furthermore, the MTJ can mature without the tendon terminating into cartilage. Based on these results, we describe a model wherein MTJ development depends on mechanical loading but not insertion into an enthesis.
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Affiliation(s)
- Sarah N Lipp
- Weldon School of Biomedical Engineering, Purdue University, 206 South Martin Jischke Drive, West Lafayette, IN 47907, United States; The Indiana University Medical Scientist/Engineer Training Program, Indianapolis, IN 46202, United States
| | - Kathryn R Jacobson
- Purdue University Interdisciplinary Life Science Program, 155 S. Grant Street, West Lafayette, IN 47907, United States
| | - Haley A Colling
- Department of Integrative Physiology, University of Colorado Boulder, 354 UCB, Boulder CO, 80309, United States
| | - Tyler G Tuttle
- Paul M. Rady Department of Mechanical Engineering, University of Colorado Boulder, 1111 Engineering Dr, Boulder, CO 80309, United States
| | - Dalton T Miles
- Chemical and Biological Engineering, University of Colorado Boulder, 596 UCB, CO 80309, United States
| | - Kaitlin P McCreery
- Paul M. Rady Department of Mechanical Engineering, University of Colorado Boulder, 1111 Engineering Dr, Boulder, CO 80309, United States
| | - Sarah Calve
- Weldon School of Biomedical Engineering, Purdue University, 206 South Martin Jischke Drive, West Lafayette, IN 47907, United States; Purdue University Interdisciplinary Life Science Program, 155 S. Grant Street, West Lafayette, IN 47907, United States; Paul M. Rady Department of Mechanical Engineering, University of Colorado Boulder, 1111 Engineering Dr, Boulder, CO 80309, United States.
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2
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Zhan YJ, Zhang SW, Zhu S, Jiang N. Tissue Clearing and Its Application in the Musculoskeletal System. ACS OMEGA 2023; 8:1739-1758. [PMID: 36687066 PMCID: PMC9850472 DOI: 10.1021/acsomega.2c05180] [Citation(s) in RCA: 0] [Impact Index Per Article: 0] [Reference Citation Analysis] [Abstract] [Grants] [Track Full Text] [Download PDF] [Figures] [Subscribe] [Scholar Register] [Received: 08/12/2022] [Accepted: 12/07/2022] [Indexed: 06/17/2023]
Abstract
The musculoskeletal system is an integral part of the human body. Currently, most skeletal muscle research is conducted through conventional histological sections due to technological limitations and the structure of skeletal muscles. For studying and observing bones and muscles, there is an urgent need for three-dimensional, objective imaging technologies. Optical tissue-clearing technologies seem to offer a novel and accessible approach to research of the musculoskeletal system. Using this approach, the components which cause refraction or prevent light from penetrating into the tissue are physically and chemically eliminated; then the liquid in the tissue is replaced with high-refractive-index chemicals. This innovative method, which allows three-dimensional reconstruction at the cellular and subcellular scale, significantly improves imaging depth and resolution. Nonetheless, this technology was not originally developed to image bones or muscles. When compared with brain and nerve organs which have attracted considerable attention in this field, the musculoskeletal system contains fewer lipids and has high levels of hemoglobin, collagen fibers, and inorganic hydroxyapatite crystals. Currently, three-dimensional imaging methods are widely used in the diagnosis and treatment of skeletal and muscular illnesses. In this regard, it is vitally important to review and evaluate the optical tissue-clearing technologies currently employed in the musculoskeletal system, so that researchers may make an informed decision. In the meantime, this study offers guidelines and recommendations for expanding the use of this technology in the musculoskeletal system.
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Affiliation(s)
- Yan-Jing Zhan
- State
Key Laboratory of Oral Diseases & National Clinical Research Center
for Oral Diseases, West China Hospital of Stomatology, Sichuan University, Chengdu 610041, China
| | - Shi-Wen Zhang
- State
Key Laboratory of Oral Diseases & National Clinical Research Center
for Oral Diseases, West China Hospital of Stomatology, Sichuan University, Chengdu 610041, China
- West
China Hospital of Stomatology, Sichuan University, Chengdu 610041, China
| | - SongSong Zhu
- State
Key Laboratory of Oral Diseases & National Clinical Research Center
for Oral Diseases, West China Hospital of Stomatology, Sichuan University, Chengdu 610041, China
- West
China Hospital of Stomatology, Sichuan University, Chengdu 610041, China
| | - Nan Jiang
- State
Key Laboratory of Oral Diseases & National Clinical Research Center
for Oral Diseases, West China Hospital of Stomatology, Sichuan University, Chengdu 610041, China
- West
China Hospital of Stomatology, Sichuan University, Chengdu 610041, China
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3
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Rubin S, Agrawal A, Stegmaier J, Krief S, Felsenthal N, Svorai J, Addadi Y, Villoutreix P, Stern T, Zelzer E. Application of 3D MAPs pipeline identifies the morphological sequence chondrocytes undergo and the regulatory role of GDF5 in this process. Nat Commun 2021; 12:5363. [PMID: 34508093 PMCID: PMC8433335 DOI: 10.1038/s41467-021-25714-0] [Citation(s) in RCA: 6] [Impact Index Per Article: 2.0] [Reference Citation Analysis] [Abstract] [Key Words] [MESH Headings] [Grants] [Track Full Text] [Download PDF] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Received: 08/28/2020] [Accepted: 08/19/2021] [Indexed: 02/08/2023] Open
Abstract
The activity of epiphyseal growth plates, which drives long bone elongation, depends on extensive changes in chondrocyte size and shape during differentiation. Here, we develop a pipeline called 3D Morphometric Analysis for Phenotypic significance (3D MAPs), which combines light-sheet microscopy, segmentation algorithms and 3D morphometric analysis to characterize morphogenetic cellular behaviors while maintaining the spatial context of the growth plate. Using 3D MAPs, we create a 3D image database of hundreds of thousands of chondrocytes. Analysis reveals broad repertoire of morphological changes, growth strategies and cell organizations during differentiation. Moreover, identifying a reduction in Smad 1/5/9 activity together with multiple abnormalities in cell growth, shape and organization provides an explanation for the shortening of Gdf5 KO tibias. Overall, our findings provide insight into the morphological sequence that chondrocytes undergo during differentiation and highlight the ability of 3D MAPs to uncover cellular mechanisms that may regulate this process.
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Affiliation(s)
- Sarah Rubin
- Department of Molecular Genetics, Weizmann Institute of Science, Rehovot, Israel
| | - Ankit Agrawal
- Department of Molecular Genetics, Weizmann Institute of Science, Rehovot, Israel
| | - Johannes Stegmaier
- Institute of Imaging and Computer Vision, RWTH Aachen University, Aachen, Germany
- Institute for Automation and Applied Informatics, Karlsruhe Institute of Technology, Karlsruhe, Germany
| | - Sharon Krief
- Department of Molecular Genetics, Weizmann Institute of Science, Rehovot, Israel
| | - Neta Felsenthal
- Department of Molecular Genetics, Weizmann Institute of Science, Rehovot, Israel
| | - Jonathan Svorai
- Department of Molecular Genetics, Weizmann Institute of Science, Rehovot, Israel
| | - Yoseph Addadi
- Department of Life Science Core Facilities, Weizmann Institute of Science, Rehovot, Israel
| | - Paul Villoutreix
- LIS (UMR 7020), IBDM (UMR 7288), Turing Center For Living Systems, Aix-Marseille University, Marseille, France.
| | - Tomer Stern
- Department of Molecular Genetics, Weizmann Institute of Science, Rehovot, Israel.
| | - Elazar Zelzer
- Department of Molecular Genetics, Weizmann Institute of Science, Rehovot, Israel.
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4
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Nowzari F, Wang H, Khoradmehr A, Baghban M, Baghban N, Arandian A, Muhaddesi M, Nabipour I, Zibaii MI, Najarasl M, Taheri P, Latifi H, Tamadon A. Three-Dimensional Imaging in Stem Cell-Based Researches. Front Vet Sci 2021; 8:657525. [PMID: 33937378 PMCID: PMC8079735 DOI: 10.3389/fvets.2021.657525] [Citation(s) in RCA: 7] [Impact Index Per Article: 2.3] [Reference Citation Analysis] [Abstract] [Key Words] [Track Full Text] [Download PDF] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Received: 01/23/2021] [Accepted: 03/19/2021] [Indexed: 12/14/2022] Open
Abstract
Stem cells have an important role in regenerative therapies, developmental biology studies and drug screening. Basic and translational research in stem cell technology needs more detailed imaging techniques. The possibility of cell-based therapeutic strategies has been validated in the stem cell field over recent years, a more detailed characterization of the properties of stem cells is needed for connectomics of large assemblies and structural analyses of these cells. The aim of stem cell imaging is the characterization of differentiation state, cellular function, purity and cell location. Recent progress in stem cell imaging field has included ultrasound-based technique to study living stem cells and florescence microscopy-based technique to investigate stem cell three-dimensional (3D) structures. Here, we summarized the fundamental characteristics of stem cells via 3D imaging methods and also discussed the emerging literatures on 3D imaging in stem cell research and the applications of both classical 2D imaging techniques and 3D methods on stem cells biology.
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Affiliation(s)
- Fariborz Nowzari
- The Persian Gulf Marine Biotechnology Research Center, The Persian Gulf Biomedical Sciences Research Institute, Bushehr University of Medical Sciences, Bushehr, Iran
| | - Huimei Wang
- Department of Integrative Medicine and Neurobiology, School of Basic Medical Sciences, Institute of Acupuncture and Moxibustion, Fudan Institutes of Integrative Medicine, Fudan University, Shanghai, China
| | - Arezoo Khoradmehr
- The Persian Gulf Marine Biotechnology Research Center, The Persian Gulf Biomedical Sciences Research Institute, Bushehr University of Medical Sciences, Bushehr, Iran
| | - Mandana Baghban
- Department of Obstetrics and Gynecology, School of Medicine, Shiraz University of Medical Sciences, Shiraz, Iran
| | - Neda Baghban
- The Persian Gulf Marine Biotechnology Research Center, The Persian Gulf Biomedical Sciences Research Institute, Bushehr University of Medical Sciences, Bushehr, Iran
| | - Alireza Arandian
- Laser and Plasma Research Institute, Shahid Beheshti University, Tehran, Iran
| | - Mahdi Muhaddesi
- The Persian Gulf Marine Biotechnology Research Center, The Persian Gulf Biomedical Sciences Research Institute, Bushehr University of Medical Sciences, Bushehr, Iran
| | - Iraj Nabipour
- The Persian Gulf Marine Biotechnology Research Center, The Persian Gulf Biomedical Sciences Research Institute, Bushehr University of Medical Sciences, Bushehr, Iran
| | - Mohammad I. Zibaii
- Laser and Plasma Research Institute, Shahid Beheshti University, Tehran, Iran
| | - Mostafa Najarasl
- Department of Stem Cells and Developmental Biology, Cell Science Research Center, Royan Institute for Stem Cell Biology and Technology, Academic Center for Education, Culture and Research (ACECR), Tehran, Iran
| | - Payam Taheri
- Department of Stem Cells and Developmental Biology, Cell Science Research Center, Royan Institute for Stem Cell Biology and Technology, Academic Center for Education, Culture and Research (ACECR), Tehran, Iran
| | - Hamid Latifi
- Laser and Plasma Research Institute, Shahid Beheshti University, Tehran, Iran
- Department of Physics, Shahid Beheshti University, Tehran, Iran
| | - Amin Tamadon
- The Persian Gulf Marine Biotechnology Research Center, The Persian Gulf Biomedical Sciences Research Institute, Bushehr University of Medical Sciences, Bushehr, Iran
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5
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Ganesh T, Laughrey LE, Niroobakhsh M, Lara-Castillo N. Multiscale finite element modeling of mechanical strains and fluid flow in osteocyte lacunocanalicular system. Bone 2020; 137:115328. [PMID: 32201360 PMCID: PMC7354216 DOI: 10.1016/j.bone.2020.115328] [Citation(s) in RCA: 17] [Impact Index Per Article: 4.3] [Reference Citation Analysis] [Abstract] [Key Words] [MESH Headings] [Grants] [Track Full Text] [Journal Information] [Submit a Manuscript] [Subscribe] [Scholar Register] [Received: 03/11/2020] [Accepted: 03/17/2020] [Indexed: 12/20/2022]
Abstract
Osteocytes form over 90% of the bone cells and are postulated to be mechanosensors responsible for regulating the function of osteoclasts and osteoblasts in bone modeling and remodeling. Physical activity results in mechanical loading on the bones. Osteocytes are thought to be the main mechanosensory cells in bone. Upon load osteocytes secrete key factors initiating downstream signaling pathways that regulate skeletal metabolism including the Wnt/β-catenin signaling pathway. Osteocytes have dendritic structures and are housed in the lacunae and canaliculi within the bone matrix. Mechanical loading is known to have two primary effects, namely a mechanical strain (membrane disruption by stretching) on the lacunae/cells, and fluid flow, in the form of fluid flow shear stress (FFSS), in the space between the cell membranes and the lacuna-canalicular walls. In response, osteocytes get activated via a process called mechanotransduction in which mechanical signals are transduced to biological responses. The study of mechanotransduction is a complex subject involving principles of engineering mechanics as well as biological signaling pathway studies. Several length scales are involved as the mechanical loading on macro sized bones are converted to strain and FFSS responses at the micro-cellular level. Experimental measurements of strain and FFSS at the cellular level are very difficult and correlating them to specific biological activity makes this a very challenging task. One of the methods commonly adopted is a multi-scale approach that combines biological and mechanical experimentation with in silico numerical modeling of the engineering aspects of the problem. Finite element analysis along with fluid-structure interaction methodologies are used to compute the mechanical strain and FFSS. These types of analyses often involve a multi-length scale approach where models of both the macro bone structure and micro structure at the cellular length scale are used. Imaging modalities play a crucial role in the development of the models and present their own challenges. This paper reviews the efforts of various research groups in addressing this problem and presents the work in our research group. A clear understanding of how mechanical stimuli affect the lacunae and perilacunar tissue strains and shear stresses on the cellular membranes may ultimately lead to a better understanding of the process of osteocyte activation.
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Affiliation(s)
- Thiagarajan Ganesh
- Department of Civil and Mechanical Engineering, University of Missouri-Kansas City, 350L Flarsheim Hall, 5100 Rockhill Road, Kansas City, MO 64110, United States of America.
| | - Loretta E Laughrey
- Department of Civil and Mechanical Engineering, University of Missouri-Kansas City, 350L Flarsheim Hall, 5100 Rockhill Road, Kansas City, MO 64110, United States of America
| | - Mohammadmehdi Niroobakhsh
- Department of Civil and Mechanical Engineering, University of Missouri-Kansas City, 350L Flarsheim Hall, 5100 Rockhill Road, Kansas City, MO 64110, United States of America
| | - Nuria Lara-Castillo
- Department of Oral and Craniofacial Sciences, School of Dentistry, University of Missouri-Kansas City, 650 E 25th Street, Kansas City, MO 64108, United States of America
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6
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Marr N, Hopkinson M, Hibbert AP, Pitsillides AA, Thorpe CT. Bimodal Whole-Mount Imaging of Tendon Using Confocal Microscopy and X-ray Micro-Computed Tomography. Biol Proced Online 2020; 22:13. [PMID: 32624710 PMCID: PMC7329428 DOI: 10.1186/s12575-020-00126-4] [Citation(s) in RCA: 8] [Impact Index Per Article: 2.0] [Reference Citation Analysis] [Abstract] [Key Words] [Track Full Text] [Download PDF] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Received: 05/06/2020] [Accepted: 06/21/2020] [Indexed: 12/25/2022] Open
Abstract
Background Three-dimensional imaging modalities for optically dense connective tissues such as tendons are limited and typically have a single imaging methodological endpoint. Here, we have developed a bimodal procedure utilising fluorescence-based confocal microscopy and x-ray micro-computed tomography for the imaging of adult tendons to visualise and analyse extracellular sub-structure and cellular composition in small and large animal species. Results Using fluorescent immunolabelling and optical clearing, we visualised the expression of the novel cross-species marker of tendon basement membrane, laminin-α4 in 3D throughout whole rat Achilles tendons and equine superficial digital flexor tendon 5 mm segments. This revealed a complex network of laminin-α4 within the tendon core that predominantly localises to the interfascicular matrix compartment. Furthermore, we implemented a chemical drying process capable of creating contrast densities enabling visualisation and quantification of both fascicular and interfascicular matrix volume and thickness by x-ray micro-computed tomography. We also demonstrated that both modalities can be combined using reverse clarification of fluorescently labelled tissues prior to chemical drying to enable bimodal imaging of a single sample. Conclusions Whole-mount imaging of tendon allowed us to identify the presence of an extensive network of laminin-α4 within tendon, the complexity of which cannot be appreciated using traditional 2D imaging techniques. Creating contrast for x-ray micro-computed tomography imaging of tendon using chemical drying is not only simple and rapid, but also markedly improves on previously published methods. Combining these methods provides the ability to gain spatio-temporal information and quantify tendon substructures to elucidate the relationship between morphology and function.
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Affiliation(s)
- Neil Marr
- Comparative Biomedical Sciences, Royal Veterinary College, Royal College Street, London, UK
| | - Mark Hopkinson
- Comparative Biomedical Sciences, Royal Veterinary College, Royal College Street, London, UK
| | - Andrew P Hibbert
- Comparative Biomedical Sciences, Royal Veterinary College, Royal College Street, London, UK
| | - Andrew A Pitsillides
- Comparative Biomedical Sciences, Royal Veterinary College, Royal College Street, London, UK
| | - Chavaunne T Thorpe
- Comparative Biomedical Sciences, Royal Veterinary College, Royal College Street, London, UK
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7
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Chaumel J, Schotte M, Bizzarro JJ, Zaslansky P, Fratzl P, Baum D, Dean MN. Co-aligned chondrocytes: Zonal morphological variation and structured arrangement of cell lacunae in tessellated cartilage. Bone 2020; 134:115264. [PMID: 32058019 DOI: 10.1016/j.bone.2020.115264] [Citation(s) in RCA: 11] [Impact Index Per Article: 2.8] [Reference Citation Analysis] [Abstract] [Key Words] [MESH Headings] [Track Full Text] [Journal Information] [Submit a Manuscript] [Subscribe] [Scholar Register] [Received: 08/15/2019] [Revised: 01/29/2020] [Accepted: 02/03/2020] [Indexed: 02/06/2023]
Abstract
In most vertebrates the embryonic cartilaginous skeleton is replaced by bone during development. During this process, cartilage cells (chondrocytes) mineralize the extracellular matrix and undergo apoptosis, giving way to bone cells (osteocytes). In contrast, sharks and rays (elasmobranchs) have cartilaginous skeletons throughout life, where only the surface mineralizes, forming a layer of tiles (tesserae). Elasmobranch chondrocytes, unlike those of other vertebrates, survive cartilage mineralization and are maintained alive in spaces (lacunae) within tesserae. However, the functions of the chondrocytes in the mineralized tissue remain unknown. Applying a custom analysis workflow to high-resolution synchrotron microCT scans of tesserae, we characterize the morphologies and arrangements of stingray chondrocyte lacunae, using lacunar morphology as a proxy for chondrocyte morphology. We show that the cell density is comparable in unmineralized and mineralized tissue and that cells maintain similar volume even when they have been incorporated into tesserae. Our findings support previous hypotheses that elasmobranch chondrocytes, unlike those of other taxa, do not proliferate, hypertrophy or undergo apoptosis during mineralization. Tessera lacunae show zonal variation in their shapes, being flatter further from and more spherical closer to the unmineralized cartilage matrix, and larger in the center of tesserae. The lacunae show pronounced organization into parallel layers and strong orientation toward neighboring tesserae. Tesserae also exhibit local variation in lacunar density, with the density considerably higher near pores passing through the tesseral layer, suggesting pores and cells interact, and that pores may contain a nutrient source. We propose that the different lacunar types reflect the stages of the tesserae formation process, while also representing local variation in tissue architecture and cell function. Lacunae are linked by small passages (canaliculi) in the matrix to form elongated series at the tesseral periphery and tight clusters in the center of tesserae, creating a rich connectivity among cells. The network arrangement and the shape variation of chondrocytes in tesserae indicate that cells may interact within and between tesserae and manage mineralization differently from chondrocytes in other vertebrates, perhaps performing analogous roles to osteocytes in bone.
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Affiliation(s)
- Júlia Chaumel
- Department of Biomaterials, Max Planck Institute of Colloids and Interfaces, Am Mühlenberg 1, 14476 Potsdam, Germany.
| | - Merlind Schotte
- Visual Data Analysis Department, Zuse Institute Berlin, Takustrasse 7, 14195 Berlin, Germany.
| | - Joseph J Bizzarro
- Institute of Marine Sciences, University of California Santa Cruz, Santa Cruz, CA, USA.
| | - Paul Zaslansky
- Department for Operative and Preventive Dentistry, Universitätsmedizin Berlin, Aßmannshauser Str. 4-6 14197 Berlin, Germany.
| | - Peter Fratzl
- Department of Biomaterials, Max Planck Institute of Colloids and Interfaces, Am Mühlenberg 1, 14476 Potsdam, Germany.
| | - Daniel Baum
- Visual Data Analysis Department, Zuse Institute Berlin, Takustrasse 7, 14195 Berlin, Germany.
| | - Mason N Dean
- Department of Biomaterials, Max Planck Institute of Colloids and Interfaces, Am Mühlenberg 1, 14476 Potsdam, Germany.
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8
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Zucchelli E, Majid QA, Foldes G. New artery of knowledge: 3D models of angiogenesis. VASCULAR BIOLOGY 2019; 1:H135-H143. [PMID: 32923965 PMCID: PMC7439835 DOI: 10.1530/vb-19-0026] [Citation(s) in RCA: 7] [Impact Index Per Article: 1.4] [Reference Citation Analysis] [Abstract] [Key Words] [Track Full Text] [Download PDF] [Figures] [Subscribe] [Scholar Register] [Received: 11/27/2019] [Accepted: 12/03/2019] [Indexed: 12/13/2022]
Abstract
Angiogenesis and vasculogenesis are complex processes by which new blood vessels are formed and expanded. They play a pivotal role not only in physiological development and growth and tissue and organ repair, but also in a range of pathological conditions, from tumour formation to chronic inflammation and atherosclerosis. Understanding the multistep cell-differentiation programmes and identifying the key molecular players of physiological angiogenesis/vasculogenesis are critical to tackle pathological mechanisms. While many questions are yet to be answered, increasingly sophisticated in vitro, in vivo and ex vivo models of angiogenesis/vasculogenesis, together with cutting-edge imaging techniques, allowed for recent major advances in the field. This review aims to summarise the three-dimensional models available to study vascular network formation and to discuss advantages and limitations of the current systems.
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Affiliation(s)
| | - Qasim A Majid
- National Heart and Lung Institute, Imperial College London, London, UK
| | - Gabor Foldes
- National Heart and Lung Institute, Imperial College London, London, UK.,Heart and Vascular Center, Semmelweis University, Budapest, Hungary
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9
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Advances toward multiscale computational models of cartilage mechanics and mechanobiology. CURRENT OPINION IN BIOMEDICAL ENGINEERING 2019. [DOI: 10.1016/j.cobme.2019.09.013] [Citation(s) in RCA: 4] [Impact Index Per Article: 0.8] [Reference Citation Analysis] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Indexed: 01/28/2023]
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10
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Urata S, Iida T, Suzuki Y, Lin SY, Mizushima Y, Fujimoto C, Matsumoto Y, Yamasoba T. A Novel Technique for Imaging and Analysis of Hair Cells in the Organ of Corti Using Modified Sca/eS and Machine Learning. Bio Protoc 2019; 9:e3342. [PMID: 33654846 DOI: 10.21769/bioprotoc.3342] [Citation(s) in RCA: 3] [Impact Index Per Article: 0.6] [Reference Citation Analysis] [Abstract] [Key Words] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Received: 05/03/2019] [Revised: 07/22/2019] [Accepted: 07/28/2019] [Indexed: 11/02/2022] Open
Abstract
Here, we describe a sorbitol-based optical clearing method, called modified Sca/eS that can be used to image all hair cells (HCs) in the mouse cochlea. This modification of Sca/eS is defined by three steps: decalcification, de-lipidation, and refractive index matching, which can all be completed within 72 h. Furthermore, we established automated analysis programs that perform machine learning-based pattern recognition. These programs generate 1) a linearized image of HCs, 2) the coordinates of HCs, 3) a holocochleogram, and 4) clusters of HC loss. In summary, a novel approach that integrates modified Sca/eS and programs based on machine learning facilitates quantitative and comprehensive analysis of the physiological and pathological properties of all HCs.
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Affiliation(s)
- Shinji Urata
- Department of Cellular Neurobiology, University of Tokyo, Tokyo, Japan.,Department of Otolaryngology, Graduate School of Medicine, University of Tokyo, Tokyo, Japan
| | - Tadatsune Iida
- Department of Cellular Neurobiology, University of Tokyo, Tokyo, Japan
| | - Yuri Suzuki
- Department of Cellular Neurobiology, University of Tokyo, Tokyo, Japan
| | - Shiou-Yuh Lin
- Department of Otolaryngology, Graduate School of Medicine, University of Tokyo, Tokyo, Japan
| | - Yu Mizushima
- Department of Otolaryngology, Graduate School of Medicine, University of Tokyo, Tokyo, Japan
| | - Chisato Fujimoto
- Department of Otolaryngology, Graduate School of Medicine, University of Tokyo, Tokyo, Japan
| | - Yu Matsumoto
- Department of Otolaryngology, Graduate School of Medicine, University of Tokyo, Tokyo, Japan
| | - Tatsuya Yamasoba
- Department of Otolaryngology, Graduate School of Medicine, University of Tokyo, Tokyo, Japan
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11
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Lycke RJ, Walls MK, Calve S. Computational Modeling of Developing Cartilage Using Experimentally Derived Geometries and Compressive Moduli. J Biomech Eng 2019; 141:081002. [PMID: 30874718 PMCID: PMC6528734 DOI: 10.1115/1.4043208] [Citation(s) in RCA: 2] [Impact Index Per Article: 0.4] [Reference Citation Analysis] [Abstract] [Grants] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Received: 05/29/2018] [Revised: 03/06/2019] [Indexed: 12/22/2022]
Abstract
During chondrogenesis, tissue organization changes dramatically. We previously showed that the compressive moduli of chondrocytes increase concomitantly with extracellular matrix (ECM) stiffness, suggesting cells were remodeling to adapt to the surrounding environment. Due to the difficulty in analyzing the mechanical response of cells in situ, we sought to create an in silico model that would enable us to investigate why cell and ECM stiffness increased in tandem. The goal of this study was to establish a methodology to segment, quantify, and generate mechanical models of developing cartilage to explore how variations in geometry and material properties affect strain distributions. Multicellular geometries from embryonic day E16.5 and postnatal day P3 murine cartilage were imaged in three-dimensional (3D) using confocal microscopy. Image stacks were processed using matlab to create geometries for finite element analysis using ANSYS. The geometries based on confocal images and isolated, single cell models were compressed 5% and the equivalent von Mises strain of cells and ECM were compared. Our simulations indicated that cells had similar strains at both time points, suggesting that the stiffness and organization of cartilage changes during development to maintain a constant strain profile within cells. In contrast, the ECM at P3 took on more strain than at E16.5. The isolated, single-cell geometries underestimated both cell and ECM strain and were not able to capture the similarity in cell strain at both time points. We expect this experimental and computational pipeline will facilitate studies investigating other model systems to implement physiologically derived geometries.
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Affiliation(s)
- Roy J Lycke
- Weldon School of Biomedical Engineering,Purdue University,206 South Martin Jischke Drive,West Lafayette, IN 47907e-mail:
| | - Michael K Walls
- Weldon School of Biomedical Engineering,Purdue University,206 South Martin Jischke Drive,West Lafayette, IN 47907e-mail:
| | - Sarah Calve
- Weldon School of Biomedical Engineering,Purdue University,206 South Martin Jischke Drive,West Lafayette, IN 47907e-mail:
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12
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Costa EC, Silva DN, Moreira AF, Correia IJ. Optical clearing methods: An overview of the techniques used for the imaging of 3D spheroids. Biotechnol Bioeng 2019; 116:2742-2763. [PMID: 31282993 DOI: 10.1002/bit.27105] [Citation(s) in RCA: 45] [Impact Index Per Article: 9.0] [Reference Citation Analysis] [Abstract] [Key Words] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Received: 02/15/2019] [Revised: 05/17/2019] [Accepted: 06/24/2019] [Indexed: 12/13/2022]
Abstract
Spheroids have emerged as in vitro models that reproduce in a great extent the architectural microenvironment found in human tissues. However, the imaging of 3D cell cultures is highly challenging due to its high thickness, which results in a light-scattering phenomenon that limits light penetration. Therefore, several optical clearing methods, widely used in the imaging of animal tissues, have been recently explored to render spheroids with enhanced transparency. These methods are aimed to homogenize the microtissue refractive index (RI) and can be grouped into four different categories, namely (a) simple immersion in an aqueous solution with high RI; (b) delipidation and dehydration followed by RI matching; (c) delipidation and hyperhydration followed by RI matching; and (d) hydrogel embedding followed by delipidation and RI matching. In this review, the main optical clearing methods, their mechanism of action, advantages, and disadvantages are described. Furthermore, the practical examples of the optical clearing methods application for the imaging of 3D spheroids are highlighted.
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Affiliation(s)
- Elisabete C Costa
- CICS-UBI, Centro de Investigação em Ciências da Saúde, Universidade da Beira Interior, Covilha, Portugal
| | - Daniel N Silva
- CICS-UBI, Centro de Investigação em Ciências da Saúde, Universidade da Beira Interior, Covilha, Portugal
| | - André F Moreira
- CICS-UBI, Centro de Investigação em Ciências da Saúde, Universidade da Beira Interior, Covilha, Portugal
| | - Ilídio J Correia
- CICS-UBI, Centro de Investigação em Ciências da Saúde, Universidade da Beira Interior, Covilha, Portugal.,CIEPQF, Departamento de Engenharia Química, Universidade de Coimbra, Coimbra, Portugal
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13
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Choi J, Lee E, Kim JH, Sun W. FxClear, A Free-hydrogel Electrophoretic Tissue Clearing Method for Rapid De-lipidation of Tissues with High Preservation of Immunoreactivity. Exp Neurobiol 2019; 28:436-445. [PMID: 31308802 PMCID: PMC6614074 DOI: 10.5607/en.2019.28.3.436] [Citation(s) in RCA: 3] [Impact Index Per Article: 0.6] [Reference Citation Analysis] [Abstract] [Key Words] [Track Full Text] [Download PDF] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Received: 03/10/2019] [Revised: 04/19/2019] [Accepted: 05/10/2019] [Indexed: 01/11/2023] Open
Abstract
Over the last two decades, several tissue clearing methodologies have been established that render tissues optically transparent and allow imaging of unsectioned tissues of significant volumes, thus improving the capacity to study the relationships between cell and 3D tissue architecture. Despite these technical advances, the important unsolved challenges that these methods face include complexity, time, consistency of tissue size before and after clearing, and ability to immunolabel various antibodies in cleared tissue. Here, we established very simple and fast tissue clearing protocol, FxClear, which involves acrylamide-free electrophoretic tissue clearing (ETC). By removal of the acrylamide infusion step, we were able to achieve fast reaction time, smaller tissue expansion, and higher immunoreactivity. Especially, immunoreactivity and fluorescence intensity were increased in FxClear-processed tissues compared to un-cleared tissues. Our protocol may be suitable for small-sized biopsy samples for 3D pathological examinations.
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Affiliation(s)
- Jungyoon Choi
- Department of Anatomy and Division of Brain Korea 21 Plus Program for Biomedical Science, Korea University College of Medicine, Seoul 02841, Korea
| | - Eunsoo Lee
- Department of Anatomy and Division of Brain Korea 21 Plus Program for Biomedical Science, Korea University College of Medicine, Seoul 02841, Korea
| | - June Hoan Kim
- Department of Anatomy and Division of Brain Korea 21 Plus Program for Biomedical Science, Korea University College of Medicine, Seoul 02841, Korea
| | - Woong Sun
- Department of Anatomy and Division of Brain Korea 21 Plus Program for Biomedical Science, Korea University College of Medicine, Seoul 02841, Korea
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14
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Jing D, Yi Y, Luo W, Zhang S, Yuan Q, Wang J, Lachika E, Zhao Z, Zhao H. Tissue Clearing and Its Application to Bone and Dental Tissues. J Dent Res 2019; 98:621-631. [PMID: 31009584 DOI: 10.1177/0022034519844510] [Citation(s) in RCA: 27] [Impact Index Per Article: 5.4] [Reference Citation Analysis] [Abstract] [Key Words] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Indexed: 02/05/2023] Open
Abstract
Opaqueness of animal tissue can be attributed mostly to light absorption and light scattering. In most noncleared tissue samples, confocal images can be acquired at no more than a 100-µm depth. Tissue-clearing techniques have emerged in recent years in the neuroscience field. Many tissue-clearing methods have been developed, and they all follow similar working principles. During the tissue-clearing process, chemical or physical treatments are applied to remove components blocking or scattering the light. Finally, samples are immersed in a designated clearing medium to achieve a uniform refractive index and to gain transparency. Once the transparency is reached, images can be acquired even at several millimeters of depth with high resolution. Tissue clearing has become an essential tool for neuroscientists to investigate the neural connectome or to analyze spatial information of various types of brain cells. Other than neural science research, tissue-clearing techniques also have applications for bone research. Several methods have been developed for clearing bones. Clearing treatment enables 3-dimensional imaging of bones without sectioning and provides important new insights that are difficult or impossible to acquire with conventional approaches. Application of tissue-clearing technique on dental research remains limited. This review will provide an overview of the recent literature related to the methods and application of various tissue-clearing methods. The following aspects will be covered: general principles for the tissue-clearing technique, current available methods for clearing bones and teeth, general principles of 3-dimensional imaging acquisition and data processing, applications of tissue clearing on studying biological processes within bones and teeth, and future directions for 3-dimensional imaging.
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Affiliation(s)
- D Jing
- 1 Department of Restorative Sciences, School of Dentistry, Texas A&M University, Dallas, TX, USA.,2 State Key Laboratory of Oral Diseases and National Clinical Research Center for Oral Diseases, West China Hospital of Stomatology, Sichuan University, Chengdu, P.R. China
| | - Y Yi
- 1 Department of Restorative Sciences, School of Dentistry, Texas A&M University, Dallas, TX, USA.,2 State Key Laboratory of Oral Diseases and National Clinical Research Center for Oral Diseases, West China Hospital of Stomatology, Sichuan University, Chengdu, P.R. China
| | - W Luo
- 1 Department of Restorative Sciences, School of Dentistry, Texas A&M University, Dallas, TX, USA
| | - S Zhang
- 2 State Key Laboratory of Oral Diseases and National Clinical Research Center for Oral Diseases, West China Hospital of Stomatology, Sichuan University, Chengdu, P.R. China
| | - Q Yuan
- 2 State Key Laboratory of Oral Diseases and National Clinical Research Center for Oral Diseases, West China Hospital of Stomatology, Sichuan University, Chengdu, P.R. China
| | - J Wang
- 2 State Key Laboratory of Oral Diseases and National Clinical Research Center for Oral Diseases, West China Hospital of Stomatology, Sichuan University, Chengdu, P.R. China
| | - E Lachika
- 3 Intelligent Imaging Innovations (3i), Denver, CO, USA
| | - Z Zhao
- 2 State Key Laboratory of Oral Diseases and National Clinical Research Center for Oral Diseases, West China Hospital of Stomatology, Sichuan University, Chengdu, P.R. China
| | - H Zhao
- 1 Department of Restorative Sciences, School of Dentistry, Texas A&M University, Dallas, TX, USA
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15
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Urata S, Iida T, Yamamoto M, Mizushima Y, Fujimoto C, Matsumoto Y, Yamasoba T, Okabe S. Cellular cartography of the organ of Corti based on optical tissue clearing and machine learning. eLife 2019; 8:40946. [PMID: 30657453 PMCID: PMC6338463 DOI: 10.7554/elife.40946] [Citation(s) in RCA: 11] [Impact Index Per Article: 2.2] [Reference Citation Analysis] [Abstract] [Key Words] [Track Full Text] [Download PDF] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Received: 08/10/2018] [Accepted: 01/05/2019] [Indexed: 12/20/2022] Open
Abstract
The highly organized spatial arrangement of sensory hair cells in the organ of Corti is essential for inner ear function. Here, we report a new analytical pipeline, based on optical clearing of tissue, for the construction of a single-cell resolution map of the organ of Corti. A sorbitol-based optical clearing method enabled imaging of the entire cochlea at subcellular resolution. High-fidelity detection and analysis of all hair cell positions along the entire longitudinal axis of the organ of Corti were performed automatically by machine learning–based pattern recognition. Application of this method to samples from young, adult, and noise-exposed mice extracted essential information regarding cellular pathology, including longitudinal and radial spatial characteristics of cell loss, implying that multiple mechanisms underlie clustered cell loss. Our method of cellular mapping is effective for system-level phenotyping of the organ of Corti under both physiological and pathological conditions.
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Affiliation(s)
- Shinji Urata
- Department of Cellular Neurobiology, Graduate School of Medicine, The University of Tokyo, Tokyo, Japan.,Department of Otolaryngology, Graduate School of Medicine, The University of Tokyo, Tokyo, Japan
| | - Tadatsune Iida
- Department of Cellular Neurobiology, Graduate School of Medicine, The University of Tokyo, Tokyo, Japan
| | - Masamichi Yamamoto
- Department of Nephrology, Graduate School of Medicine, Kyoto University, Kyoto, Japan
| | - Yu Mizushima
- Department of Otolaryngology, Graduate School of Medicine, The University of Tokyo, Tokyo, Japan
| | - Chisato Fujimoto
- Department of Otolaryngology, Graduate School of Medicine, The University of Tokyo, Tokyo, Japan
| | - Yu Matsumoto
- Department of Otolaryngology, Graduate School of Medicine, The University of Tokyo, Tokyo, Japan
| | - Tatsuya Yamasoba
- Department of Otolaryngology, Graduate School of Medicine, The University of Tokyo, Tokyo, Japan
| | - Shigeo Okabe
- Department of Cellular Neurobiology, Graduate School of Medicine, The University of Tokyo, Tokyo, Japan
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16
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Noë M, Rezaee N, Asrani K, Skaro M, Groot VP, Wu PH, Olson MT, Hong SM, Kim SJ, Weiss MJ, Wolfgang CL, Makary MA, He J, Cameron JL, Wirtz D, Roberts NJ, Offerhaus GJA, Brosens LAA, Wood LD, Hruban RH. Immunolabeling of Cleared Human Pancreata Provides Insights into Three-Dimensional Pancreatic Anatomy and Pathology. THE AMERICAN JOURNAL OF PATHOLOGY 2018; 188:1530-1535. [PMID: 29684363 PMCID: PMC6024186 DOI: 10.1016/j.ajpath.2018.04.002] [Citation(s) in RCA: 28] [Impact Index Per Article: 4.7] [Reference Citation Analysis] [Abstract] [MESH Headings] [Grants] [Track Full Text] [Subscribe] [Scholar Register] [Received: 01/02/2018] [Revised: 03/29/2018] [Accepted: 04/02/2018] [Indexed: 11/22/2022]
Abstract
Visualizing pathologies in three dimensions can provide unique insights into the biology of human diseases. A rapid and easy-to-implement dibenzyl ether-based technique was used to clear thick sections of surgically resected human pancreatic parenchyma. Protocols were applicable to both fresh and formalin-fixed, paraffin-embedded tissue. The penetration of antibodies into dense pancreatic parenchyma was optimized using both gradually increasing antibody concentrations and centrifugal flow. Immunolabeling with antibodies against cytokeratin 19 was visualized using both light sheet and confocal laser scanning microscopy. The technique was applied successfully to 26 sections of pancreas, providing three-dimensional (3D) images of normal pancreatic tissue, pancreatic intraepithelial neoplasia, intraductal papillary mucinous neoplasms, and infiltrating pancreatic ductal adenocarcinomas. 3D visualization highlighted processes that are hard to conceptualize in two dimensions, such as invasive carcinoma growing into what appeared to be pre-existing pancreatic ducts and within venules, and the tracking of long cords of neoplastic cells parallel to blood vessels. Expanding this technique to formalin-fixed, paraffin-embedded tissue opens pathology archives to 3D visualization of unique biosamples and rare diseases. The application of immunolabeling and clearing to human pancreatic parenchyma provides detailed visualization of normal pancreatic anatomy, and can be used to characterize the 3D architecture of diseases including pancreatic intraepithelial neoplasia, intraductal papillary mucinous neoplasm, and pancreatic ductal adenocarcinomas.
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Affiliation(s)
- Michaël Noë
- Department of Pathology, Sol Goldman Pancreatic Cancer Research Center, Johns Hopkins University School of Medicine, Baltimore, Maryland; Department of Oncology, Sol Goldman Pancreatic Cancer Research Center, Johns Hopkins University School of Medicine, Baltimore, Maryland
| | - Neda Rezaee
- Department of Surgery, Sol Goldman Pancreatic Cancer Research Center, Johns Hopkins University School of Medicine, Baltimore, Maryland
| | - Kaushal Asrani
- Department of Pathology, Sol Goldman Pancreatic Cancer Research Center, Johns Hopkins University School of Medicine, Baltimore, Maryland
| | - Michael Skaro
- Department of Pathology, Sol Goldman Pancreatic Cancer Research Center, Johns Hopkins University School of Medicine, Baltimore, Maryland
| | - Vincent P Groot
- Department of Surgery, Sol Goldman Pancreatic Cancer Research Center, Johns Hopkins University School of Medicine, Baltimore, Maryland
| | - Pei-Hsun Wu
- Department of Chemical and Biomolecular Engineering, Johns Hopkins University, Baltimore, Maryland
| | - Matthew T Olson
- Department of Pathology, Sol Goldman Pancreatic Cancer Research Center, Johns Hopkins University School of Medicine, Baltimore, Maryland
| | - Seung-Mo Hong
- Department of Pathology, Asan Medical Center, University of Ulsan College of Medicine, Seoul, Republic of Korea
| | - Sung Joo Kim
- Department of Pathology, Asan Medical Center, University of Ulsan College of Medicine, Seoul, Republic of Korea
| | - Matthew J Weiss
- Department of Surgery, Sol Goldman Pancreatic Cancer Research Center, Johns Hopkins University School of Medicine, Baltimore, Maryland
| | - Christopher L Wolfgang
- Department of Surgery, Sol Goldman Pancreatic Cancer Research Center, Johns Hopkins University School of Medicine, Baltimore, Maryland
| | - Martin A Makary
- Department of Surgery, Sol Goldman Pancreatic Cancer Research Center, Johns Hopkins University School of Medicine, Baltimore, Maryland
| | - Jin He
- Department of Surgery, Sol Goldman Pancreatic Cancer Research Center, Johns Hopkins University School of Medicine, Baltimore, Maryland
| | - John L Cameron
- Department of Surgery, Sol Goldman Pancreatic Cancer Research Center, Johns Hopkins University School of Medicine, Baltimore, Maryland
| | - Denis Wirtz
- Department of Pathology, Sol Goldman Pancreatic Cancer Research Center, Johns Hopkins University School of Medicine, Baltimore, Maryland; Department of Chemical and Biomolecular Engineering, Johns Hopkins University, Baltimore, Maryland
| | - Nicholas J Roberts
- Department of Pathology, Sol Goldman Pancreatic Cancer Research Center, Johns Hopkins University School of Medicine, Baltimore, Maryland; Department of Oncology, Sol Goldman Pancreatic Cancer Research Center, Johns Hopkins University School of Medicine, Baltimore, Maryland
| | - G Johan A Offerhaus
- Department of Pathology, University Medical Center Utrecht, Utrecht, the Netherlands
| | - Lodewijk A A Brosens
- Department of Pathology, University Medical Center Utrecht, Utrecht, the Netherlands
| | - Laura D Wood
- Department of Pathology, Sol Goldman Pancreatic Cancer Research Center, Johns Hopkins University School of Medicine, Baltimore, Maryland; Department of Oncology, Sol Goldman Pancreatic Cancer Research Center, Johns Hopkins University School of Medicine, Baltimore, Maryland.
| | - Ralph H Hruban
- Department of Pathology, Sol Goldman Pancreatic Cancer Research Center, Johns Hopkins University School of Medicine, Baltimore, Maryland; Department of Oncology, Sol Goldman Pancreatic Cancer Research Center, Johns Hopkins University School of Medicine, Baltimore, Maryland.
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17
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Acuna A, Drakopoulos MA, Leng Y, Goergen CJ, Calve S. Three-dimensional visualization of extracellular matrix networks during murine development. Dev Biol 2018; 435:122-129. [PMID: 29352963 PMCID: PMC6097807 DOI: 10.1016/j.ydbio.2017.12.022] [Citation(s) in RCA: 13] [Impact Index Per Article: 2.2] [Reference Citation Analysis] [Abstract] [Key Words] [MESH Headings] [Grants] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Received: 08/10/2017] [Revised: 12/16/2017] [Accepted: 12/30/2017] [Indexed: 11/15/2022]
Abstract
The extracellular matrix (ECM) plays a crucial role in embryogenesis, serving both as a substrate to which cells attach and as an active regulator of cell behavior. However, little is known about the spatiotemporal expression patterns and 3D structure of ECM proteins during embryonic development. The lack of suitable methods to visualize the embryonic ECM is largely responsible for this gap, posing a major technical challenge for biologists and tissue engineers. Here, we describe a method of viewing the 3D organization of the ECM using a polyacrylamide-based hydrogel to provide a 3D framework within developing murine embryos. After removal of soluble proteins using sodium dodecyl sulfate, confocal microscopy was used to visualize the 3D distribution of independent ECM networks in multiple developing tissues, including the forelimb, eye, and spinal cord. Comparative analysis of E12.5 and E14.5 autopods revealed proteoglycan-rich fibrils maintain connections between the epidermis and the underlying tendon and cartilage, indicating a role for the ECM during musculoskeletal assembly and demonstrating that our method can be a powerful tool for defining the spatiotemporal distribution of the ECM during embryogenesis.
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Affiliation(s)
- Andrea Acuna
- Weldon School of Biomedical Engineering, Purdue University, 206 South Martin Jischke Drive, West Lafayette, IN 47907, USA
| | - Michael A Drakopoulos
- Weldon School of Biomedical Engineering, Purdue University, 206 South Martin Jischke Drive, West Lafayette, IN 47907, USA
| | - Yue Leng
- Weldon School of Biomedical Engineering, Purdue University, 206 South Martin Jischke Drive, West Lafayette, IN 47907, USA
| | - Craig J Goergen
- Weldon School of Biomedical Engineering, Purdue University, 206 South Martin Jischke Drive, West Lafayette, IN 47907, USA
| | - Sarah Calve
- Weldon School of Biomedical Engineering, Purdue University, 206 South Martin Jischke Drive, West Lafayette, IN 47907, USA.
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18
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Alexandrovskaya Y, Sadovnikov K, Sharov A, Sherstneva A, Evtushenko E, Omelchenko A, Obrezkova M, Tuchin V, Lunin V, Sobol E. Controlling the near-infrared transparency of costal cartilage by impregnation with clearing agents and magnetite nanoparticles. JOURNAL OF BIOPHOTONICS 2018; 11:e201700105. [PMID: 28731618 DOI: 10.1002/jbio.201700105] [Citation(s) in RCA: 3] [Impact Index Per Article: 0.5] [Reference Citation Analysis] [Abstract] [Key Words] [MESH Headings] [Track Full Text] [Subscribe] [Scholar Register] [Received: 04/28/2017] [Revised: 07/18/2017] [Accepted: 07/19/2017] [Indexed: 06/07/2023]
Abstract
Penetration depth of near-infrared laser radiation to costal cartilage is controlled by the tissue absorption and scattering, and it is the critical parameter to provide the relaxation of mechanical stress throughout the whole thickness of cartilage implant. To enhance the penetration for the laser radiation on 1.56 μm, the optical clearing solutions of glycerol and fructose of various concentrations are tested. The effective and reversible tissue clearance was achieved. However, the increasing absorption of radiation should be concerned: 5°C-8°C increase of tissue temperature was detected. Laser parameters used for stress relaxation in cartilage should be optimized when applying optical clearing agents. To concentrate the absorption in the superficial tissue layers, magnetite nanoparticle (NP) dispersions with the mean size 95 ± 5 nm and concentration 3.9 ± 1.1 × 1011 particles/mL are applied. The significant increase in the tissue heating rate was observed along with the decrease in its transparency. Using NPs the respective laser power can be decreased, allowing us to obtain the working temperature locally with reduced thermal effect on the surrounding tissue.
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Affiliation(s)
- Yulia Alexandrovskaya
- Institute of Applied Physics of the Russian Academy of Sciences, Nizhny Novgorod, Russia
- Institute of Photon Technologies, Federal Scientific Research Centre "Crystallography and Photonics" of the Russian Academy of Sciences, Moscow, Russia
- M.V. Lomonosov Moscow State University, Moscow, Russia
| | | | - Andrey Sharov
- M.V. Lomonosov Moscow State University, Moscow, Russia
| | | | | | - Alexander Omelchenko
- Institute of Applied Physics of the Russian Academy of Sciences, Nizhny Novgorod, Russia
- Institute of Photon Technologies, Federal Scientific Research Centre "Crystallography and Photonics" of the Russian Academy of Sciences, Moscow, Russia
| | | | - Valery Tuchin
- Research-Educational Institute of Optics and Biophotonics, National Research Saratov State University, Saratov, Russia
- Laboratory of Laser Diagnostics of Technical and Living Systems, Institute of Precision Mechanics and Control RAS, Saratov, Russia
- Interdisciplinary Laboratory of Biophotonics, National Research Tomsk State University, Tomsk, Russia
| | - Valery Lunin
- M.V. Lomonosov Moscow State University, Moscow, Russia
| | - Emil Sobol
- Institute of Applied Physics of the Russian Academy of Sciences, Nizhny Novgorod, Russia
- Institute of Photon Technologies, Federal Scientific Research Centre "Crystallography and Photonics" of the Russian Academy of Sciences, Moscow, Russia
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19
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Chan DD, Cai L, Butz KD, Nauman EA, Dickerson DA, Jonkers I, Neu CP. Functional MRI can detect changes in intratissue strains in a full thickness and critical sized ovine cartilage defect model. J Biomech 2018; 66:18-25. [PMID: 29169631 PMCID: PMC5767131 DOI: 10.1016/j.jbiomech.2017.10.031] [Citation(s) in RCA: 12] [Impact Index Per Article: 2.0] [Reference Citation Analysis] [Abstract] [Key Words] [MESH Headings] [Grants] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Received: 06/23/2017] [Revised: 10/02/2017] [Accepted: 10/27/2017] [Indexed: 02/07/2023]
Abstract
Functional imaging of tissue biomechanics can reveal subtle changes in local softening and stiffening associated with disease or repair, but noninvasive and nondestructive methods to acquire intratissue measures in well-defined animal models are largely lacking. We utilized displacement encoded MRI to measure changes in cartilage deformation following creation of a critical-sized defect in the medial femoral condyle of ovine (sheep) knees, a common in situ and large animal model of tissue damage and repair. We prioritized visualization of local, site-specific variation and changes in displacements and strains following defect placement by measuring spatial maps of intratissue deformation. Custom data smoothing algorithms were developed to minimize propagation of noise in the acquired MRI phase data toward calculated displacement or strain, and to improve strain measures in high aspect ratio tissue regions. Strain magnitudes in the femoral, but not tibial, cartilage dramatically increased in load-bearing and contact regions especially near the defect locations, with an average 6.7% ± 6.3%, 13.4% ± 10.0%, and 10.0% ± 4.9% increase in first and second principal strains, and shear strain, respectively. Strain heterogeneity reflected the complexity of the in situ mechanical environment within the joint, with multiple tissue contacts defining the deformation behavior. This study demonstrates the utility of displacement encoded MRI to detect increased deformation patterns and strain following disruption to the cartilage structure in a clinically-relevant, large animal defect model. It also defines imaging biomarkers based on biomechanical measures, in particular shear strain, that are potentially most sensitive to evaluate damage and repair, and that may additionally translate to humans in future studies.
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Affiliation(s)
- Deva D Chan
- Weldon School of Biomedical Engineering, Purdue University, West Lafayette, IN 47907, United States; Department of Biomedical Engineering, Rensselaer Polytechnic Institute, Troy, NY 12180, United States
| | - Luyao Cai
- Weldon School of Biomedical Engineering, Purdue University, West Lafayette, IN 47907, United States
| | - Kent D Butz
- School of Mechanical Engineering, Purdue University, West Lafayette, IN 47907, United States
| | - Eric A Nauman
- Weldon School of Biomedical Engineering, Purdue University, West Lafayette, IN 47907, United States; School of Mechanical Engineering, Purdue University, West Lafayette, IN 47907, United States; BioRegeneration Technologies, Inc., West Lafayette, IN 47907, United States
| | - Darryl A Dickerson
- School of Mechanical Engineering, Purdue University, West Lafayette, IN 47907, United States; BioRegeneration Technologies, Inc., West Lafayette, IN 47907, United States
| | - Ilse Jonkers
- Kinesiology Department, KU Leuven, Leuven, Belgium
| | - Corey P Neu
- Weldon School of Biomedical Engineering, Purdue University, West Lafayette, IN 47907, United States; Department of Mechanical Engineering, University of Colorado Boulder, Boulder, CO 80309, United States.
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20
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Mayrand D, Fradette J. High Definition Confocal Imaging Modalities for the Characterization of Tissue-Engineered Substitutes. Methods Mol Biol 2018; 1773:93-105. [PMID: 29687383 DOI: 10.1007/978-1-4939-7799-4_8] [Citation(s) in RCA: 3] [Impact Index Per Article: 0.5] [Reference Citation Analysis] [Abstract] [Key Words] [MESH Headings] [Grants] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Indexed: 06/08/2023]
Abstract
Optimal imaging methods are necessary in order to perform a detailed characterization of thick tissue samples from either native or engineered tissues. Tissue-engineered substitutes are featuring increasing complexity including multiple cell types and capillary-like networks. Therefore, technical approaches allowing the visualization of the inner structural organization and cellular composition of tissues are needed. This chapter describes an optical clearing technique which facilitates the detailed characterization of whole-mount samples from skin and adipose tissues (ex vivo tissues and in vitro tissue-engineered substitutes) when combined with spectral confocal microscopy and quantitative analysis on image renderings.
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Affiliation(s)
- Dominique Mayrand
- Centre de Recherche en Organogénèse Expérimentale de l'Université Laval/LOEX, CRCHU de Québec-Université Laval, Québec, QC, Canada
- Department of Surgery, Faculty of Medicine, Université Laval, Québec, QC, Canada
| | - Julie Fradette
- Centre de Recherche en Organogénèse Expérimentale de l'Université Laval/LOEX, CRCHU de Québec-Université Laval, Québec, QC, Canada.
- Department of Surgery, Faculty of Medicine, Université Laval, Québec, QC, Canada.
- CMDGT/LOEX, Aile-R, Pavilion Hôpital Enfant-Jésus, CRCHU de Québec-Université Laval, Québec, QC, Canada.
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21
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Jensen KHR, Berg RW. Advances and perspectives in tissue clearing using CLARITY. J Chem Neuroanat 2017; 86:19-34. [DOI: 10.1016/j.jchemneu.2017.07.005] [Citation(s) in RCA: 34] [Impact Index Per Article: 4.9] [Reference Citation Analysis] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Received: 05/23/2017] [Revised: 07/12/2017] [Accepted: 07/12/2017] [Indexed: 12/16/2022]
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22
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Zeller-Plumhoff B, Roose T, Clough GF, Schneider P. Image-based modelling of skeletal muscle oxygenation. J R Soc Interface 2017; 14:rsif.2016.0992. [PMID: 28202595 DOI: 10.1098/rsif.2016.0992] [Citation(s) in RCA: 13] [Impact Index Per Article: 1.9] [Reference Citation Analysis] [Abstract] [Key Words] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Received: 12/08/2016] [Accepted: 01/25/2017] [Indexed: 12/12/2022] Open
Abstract
The supply of oxygen in sufficient quantity is vital for the correct functioning of all organs in the human body, in particular for skeletal muscle during exercise. Disease is often associated with both an inhibition of the microvascular supply capability and is thought to relate to changes in the structure of blood vessel networks. Different methods exist to investigate the influence of the microvascular structure on tissue oxygenation, varying over a range of application areas, i.e. biological in vivo and in vitro experiments, imaging and mathematical modelling. Ideally, all of these methods should be combined within the same framework in order to fully understand the processes involved. This review discusses the mathematical models of skeletal muscle oxygenation currently available that are based upon images taken of the muscle microvasculature in vivo and ex vivo Imaging systems suitable for capturing the blood vessel networks are discussed and respective contrasting methods presented. The review further informs the association between anatomical characteristics in health and disease. With this review we give the reader a tool to understand and establish the workflow of developing an image-based model of skeletal muscle oxygenation. Finally, we give an outlook for improvements needed for measurements and imaging techniques to adequately investigate the microvascular capability for oxygen exchange.
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Affiliation(s)
- B Zeller-Plumhoff
- Helmholtz-Zentrum für Material- und Küstenforschung, Geesthacht, Germany .,Bioengineering Research Group, Faculty of Engineering and the Environment, University of Southampton, Southampton, UK
| | - T Roose
- Bioengineering Research Group, Faculty of Engineering and the Environment, University of Southampton, Southampton, UK
| | - G F Clough
- Faculty of Medicine, University of Southampton, Southampton, UK
| | - P Schneider
- Bioengineering Research Group, Faculty of Engineering and the Environment, University of Southampton, Southampton, UK
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23
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Greenbaum A, Chan KY, Dobreva T, Brown D, Balani DH, Boyce R, Kronenberg HM, McBride HJ, Gradinaru V. Bone CLARITY: Clearing, imaging, and computational analysis of osteoprogenitors within intact bone marrow. Sci Transl Med 2017; 9:9/387/eaah6518. [DOI: 10.1126/scitranslmed.aah6518] [Citation(s) in RCA: 120] [Impact Index Per Article: 17.1] [Reference Citation Analysis] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Received: 07/27/2016] [Accepted: 03/23/2017] [Indexed: 12/14/2022]
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24
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Løvdal ALV, Calve S, Yang S, Van Alstine W, Binkert CA, Klausen K. Evaluation of a Bioabsorbable Self-Expandable Vein Stent-Base Made of Poly(l-lactide) In Vitro and In Vivo. Cardiovasc Intervent Radiol 2016; 40:112-119. [DOI: 10.1007/s00270-016-1491-2] [Citation(s) in RCA: 3] [Impact Index Per Article: 0.4] [Reference Citation Analysis] [Track Full Text] [Journal Information] [Submit a Manuscript] [Subscribe] [Scholar Register] [Received: 06/17/2016] [Accepted: 10/26/2016] [Indexed: 11/30/2022]
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25
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Pires L, Demidov V, Vitkin IA, Bagnato V, Kurachi C, Wilson BC. Optical clearing of melanoma in vivo: characterization by diffuse reflectance spectroscopy and optical coherence tomography. JOURNAL OF BIOMEDICAL OPTICS 2016; 21:081210. [PMID: 27300502 DOI: 10.1117/1.jbo.21.8.081210] [Citation(s) in RCA: 13] [Impact Index Per Article: 1.6] [Reference Citation Analysis] [Abstract] [MESH Headings] [Track Full Text] [Subscribe] [Scholar Register] [Received: 02/16/2016] [Accepted: 05/23/2016] [Indexed: 05/03/2023]
Abstract
Melanoma is the most aggressive type of skin cancer, with significant risk of fatality. Due to its pigmentation, light-based imaging and treatment techniques are limited to near the tumor surface, which is inadequate, for example, to evaluate the microvascular density that is associated with prognosis. White-light diffuse reflectance spectroscopy (DRS) and near-infrared optical coherence tomography (OCT) were used to evaluate the effect of a topically applied optical clearing agent (OCA) in melanoma in vivo and to image the microvascular network. DRS was performed using a contact fiber optic probe in the range from 450 to 650 nm. OCT imaging was performed using a swept-source system at 1310 nm. The OCT image data were processed using speckle variance and depth-encoded algorithms. Diffuse reflectance signals decreased with clearing, dropping by ∼ 90% after 45 min. OCT was able to image the microvasculature in the pigmented melanoma tissue with good spatial resolution up to a depth of ∼ 300 μm without the use of OCA; improved contrast resolution was achieved with optical clearing to a depth of ∼ 750 μm in tumor. These findings are relevant to potential clinical applications in melanoma, such as assessing prognosis and treatment responses. Optical clearing may also facilitate the use of light-based treatments such as photodynamic therapy.
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Affiliation(s)
- Layla Pires
- University of São Paulo, São Carlos Institute of Physics, Avenue Trabalhador São-Carlense, 400, São Carlos, São Paulo 13566-590, BrazilbUniversity of Toronto, Department of Medical Biophysics, Princess Margaret Cancer Research Tower, 101 College Street, T
| | - Valentin Demidov
- University of Toronto, Department of Medical Biophysics, Princess Margaret Cancer Research Tower, 101 College Street, Toronto, Ontario M5G 1L7, Canada
| | - I Alex Vitkin
- University of Toronto, Department of Medical Biophysics, Princess Margaret Cancer Research Tower, 101 College Street, Toronto, Ontario M5G 1L7, CanadacUniversity Health Network, Princess Margaret Cancer Center, Princess Margaret Cancer Research Tower, 101
| | - Vanderlei Bagnato
- University of São Paulo, São Carlos Institute of Physics, Avenue Trabalhador São-Carlense, 400, São Carlos, São Paulo 13566-590, Brazil
| | - Cristina Kurachi
- University of São Paulo, São Carlos Institute of Physics, Avenue Trabalhador São-Carlense, 400, São Carlos, São Paulo 13566-590, Brazil
| | - Brian C Wilson
- University of Toronto, Department of Medical Biophysics, Princess Margaret Cancer Research Tower, 101 College Street, Toronto, Ontario M5G 1L7, CanadacUniversity Health Network, Princess Margaret Cancer Center, Princess Margaret Cancer Research Tower, 101
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26
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Treweek JB, Gradinaru V. Extracting structural and functional features of widely distributed biological circuits with single cell resolution via tissue clearing and delivery vectors. Curr Opin Biotechnol 2016; 40:193-207. [PMID: 27393829 DOI: 10.1016/j.copbio.2016.03.012] [Citation(s) in RCA: 37] [Impact Index Per Article: 4.6] [Reference Citation Analysis] [Abstract] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Received: 11/16/2015] [Revised: 03/10/2016] [Accepted: 03/15/2016] [Indexed: 12/13/2022]
Abstract
The scientific community has learned a great deal from imaging small and naturally transparent organisms such as nematodes and zebrafish. The consequences of genetic mutations on their organ development and survival can be visualized easily and with high-throughput at the organism-wide scale. In contrast, three-dimensional information is less accessible in mammalian subjects because the heterogeneity of light-scattering tissue elements renders their organs opaque. Likewise, genetically labeling desired circuits across mammalian bodies is prohibitively slow and costly via the transgenic route. Emerging breakthroughs in viral vector engineering, genome editing tools, and tissue clearing can render larger opaque organisms genetically tractable and transparent for whole-organ cell phenotyping, tract tracing and imaging at depth.
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Affiliation(s)
- Jennifer Brooke Treweek
- Division of Biology and Biological Engineering, California Institute of Technology, Pasadena, CA, USA
| | - Viviana Gradinaru
- Division of Biology and Biological Engineering, California Institute of Technology, Pasadena, CA, USA.
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Azaripour A, Lagerweij T, Scharfbillig C, Jadczak AE, Willershausen B, Van Noorden CJF. A survey of clearing techniques for 3D imaging of tissues with special reference to connective tissue. ACTA ACUST UNITED AC 2016; 51:9-23. [PMID: 27142295 DOI: 10.1016/j.proghi.2016.04.001] [Citation(s) in RCA: 108] [Impact Index Per Article: 13.5] [Reference Citation Analysis] [Abstract] [Key Words] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Received: 03/30/2016] [Revised: 04/07/2016] [Accepted: 04/11/2016] [Indexed: 11/25/2022]
Abstract
For 3-dimensional (3D) imaging of a tissue, 3 methodological steps are essential and their successful application depends on specific characteristics of the type of tissue. The steps are 1° clearing of the opaque tissue to render it transparent for microscopy, 2° fluorescence labeling of the tissues and 3° 3D imaging. In the past decades, new methodologies were introduced for the clearing steps with their specific advantages and disadvantages. Most clearing techniques have been applied to the central nervous system and other organs that contain relatively low amounts of connective tissue including extracellular matrix. However, tissues that contain large amounts of extracellular matrix such as dermis in skin or gingiva are difficult to clear. The present survey lists methodologies that are available for clearing of tissues for 3D imaging. We report here that the BABB method using a mixture of benzyl alcohol and benzyl benzoate and iDISCO using dibenzylether (DBE) are the most successful methods for clearing connective tissue-rich gingiva and dermis of skin for 3D histochemistry and imaging of fluorescence using light-sheet microscopy.
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Affiliation(s)
- Adriano Azaripour
- Department of Operative Dentistry, University Medical Center of the Johannes Gutenberg University Mainz, Augustusplatz 2, Mainz 55131, Germany; Department of Cell Biology and Histology, Academic Medical Center, University of Amsterdam, Meibergdreef 15, 1105 AZ Amsterdam, The Netherlands.
| | - Tonny Lagerweij
- Neuro-Oncology Research Group, VU University Medical Center, Cancer Center Amsterdam, Room 3.20, De Boelelaan 1117, 1081 HV Amsterdam, The Netherlands
| | - Christina Scharfbillig
- Department of Operative Dentistry, University Medical Center of the Johannes Gutenberg University Mainz, Augustusplatz 2, Mainz 55131, Germany
| | - Anna Elisabeth Jadczak
- Department of Operative Dentistry, University Medical Center of the Johannes Gutenberg University Mainz, Augustusplatz 2, Mainz 55131, Germany
| | - Brita Willershausen
- Department of Operative Dentistry, University Medical Center of the Johannes Gutenberg University Mainz, Augustusplatz 2, Mainz 55131, Germany
| | - Cornelis J F Van Noorden
- Department of Cell Biology and Histology, Academic Medical Center, University of Amsterdam, Meibergdreef 15, 1105 AZ Amsterdam, The Netherlands
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28
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Berke IM, Miola JP, David MA, Smith MK, Price C. Seeing through Musculoskeletal Tissues: Improving In Situ Imaging of Bone and the Lacunar Canalicular System through Optical Clearing. PLoS One 2016; 11:e0150268. [PMID: 26930293 PMCID: PMC4773178 DOI: 10.1371/journal.pone.0150268] [Citation(s) in RCA: 36] [Impact Index Per Article: 4.5] [Reference Citation Analysis] [Abstract] [MESH Headings] [Grants] [Track Full Text] [Download PDF] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Received: 09/15/2015] [Accepted: 02/11/2016] [Indexed: 12/17/2022] Open
Abstract
In situ, cells of the musculoskeletal system reside within complex and often interconnected 3-D environments. Key to better understanding how 3-D tissue and cellular environments regulate musculoskeletal physiology, homeostasis, and health is the use of robust methodologies for directly visualizing cell-cell and cell-matrix architecture in situ. However, the use of standard optical imaging techniques is often of limited utility in deep imaging of intact musculoskeletal tissues due to the highly scattering nature of biological tissues. Drawing inspiration from recent developments in the deep-tissue imaging field, we describe the application of immersion based optical clearing techniques, which utilize the principle of refractive index (RI) matching between the clearing/mounting media and tissue under observation, to improve the deep, in situ imaging of musculoskeletal tissues. To date, few optical clearing techniques have been applied specifically to musculoskeletal tissues, and a systematic comparison of the clearing ability of optical clearing agents in musculoskeletal tissues has yet to be fully demonstrated. In this study we tested the ability of eight different aqueous and non-aqueous clearing agents, with RIs ranging from 1.45 to 1.56, to optically clear murine knee joints and cortical bone. We demonstrated and quantified the ability of these optical clearing agents to clear musculoskeletal tissues and improve both macro- and micro-scale imaging of musculoskeletal tissue across several imaging modalities (stereomicroscopy, spectroscopy, and one-, and two-photon confocal microscopy) and investigational techniques (dynamic bone labeling and en bloc tissue staining). Based upon these findings we believe that optical clearing, in combination with advanced imaging techniques, has the potential to complement classical musculoskeletal analysis techniques; opening the door for improved in situ investigation and quantification of musculoskeletal tissues.
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Affiliation(s)
- Ian M. Berke
- Department of Biomedical Engineering, University of Delaware, Newark, Delaware, United States of America
| | - Joseph P. Miola
- Department of Biomedical Engineering, University of Delaware, Newark, Delaware, United States of America
| | - Michael A. David
- Department of Biomedical Engineering, University of Delaware, Newark, Delaware, United States of America
| | - Melanie K. Smith
- Department of Biomedical Engineering, University of Delaware, Newark, Delaware, United States of America
| | - Christopher Price
- Department of Biomedical Engineering, University of Delaware, Newark, Delaware, United States of America
- * E-mail:
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Milgroom A, Ralston E. Clearing skeletal muscle with CLARITY for light microscopy imaging. Cell Biol Int 2016; 40:478-83. [PMID: 26732743 DOI: 10.1002/cbin.10578] [Citation(s) in RCA: 16] [Impact Index Per Article: 2.0] [Reference Citation Analysis] [Abstract] [Key Words] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Received: 10/14/2015] [Accepted: 12/30/2015] [Indexed: 11/09/2022]
Abstract
Viewing subcellular details over large tissue volumes is becoming an essential condition of the success of large-scale projects aimed at visualizing cell connections in whole organs or tissues. However, tissue opacity remains an obstacle to deep tissue imaging. This situation has brought renewed interest for techniques of tissue clearing; new protocols, such as CLARITY (Clear Lipid-exchanged Acrylamide-hybridized Rigid Imaging/Immunostaining/In situ hybridization-compatible Tissue-hYdrogel), have recently been developed. So far, most of the tests of these techniques have been applied to brain or other soft tissues. Here we show that CLARITY clears mouse hindlimb skeletal muscles and maintains the basic structural features of muscle and its fibers. However, tagging with fluorescent markers was not successful.
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Affiliation(s)
- Andrew Milgroom
- Light Imaging Section, Office of Science and Technology, National Institute of Arthritis and Musculoskeletal and Skin Diseases, National Institutes of Health, Bethesda, Maryland, 20892-8023, USA
| | - Evelyn Ralston
- Light Imaging Section, Office of Science and Technology, National Institute of Arthritis and Musculoskeletal and Skin Diseases, National Institutes of Health, Bethesda, Maryland, 20892-8023, USA
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30
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Application of Elastography for the Noninvasive Assessment of Biomechanics in Engineered Biomaterials and Tissues. Ann Biomed Eng 2016; 44:705-24. [PMID: 26790865 DOI: 10.1007/s10439-015-1542-x] [Citation(s) in RCA: 18] [Impact Index Per Article: 2.3] [Reference Citation Analysis] [Abstract] [Key Words] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Received: 09/29/2015] [Accepted: 12/18/2015] [Indexed: 12/11/2022]
Abstract
The elastic properties of engineered biomaterials and tissues impact their post-implantation repair potential and structural integrity, and are critical to help regulate cell fate and gene expression. The measurement of properties (e.g., stiffness or shear modulus) can be attained using elastography, which exploits noninvasive imaging modalities to provide functional information of a material indicative of the regeneration state. In this review, we outline the current leading elastography methodologies available to characterize the properties of biomaterials and tissues suitable for repair and mechanobiology research. We describe methods utilizing magnetic resonance, ultrasound, and optical coherent elastography, highlighting their potential for longitudinal monitoring of implanted materials in vivo, in addition to spatiotemporal limits of each method for probing changes in cell-laden constructs. Micro-elastography methods now allow acquisitions at length scales approaching 5-100 μm in two and three dimensions. Many of the methods introduced in this review are therefore capable of longitudinal monitoring in biomaterials and tissues approaching the cellular scale. However, critical factors such as anisotropy, heterogeneity and viscoelasity-inherent in many soft tissues-are often not fully described and therefore require further advancements and future developments.
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Lee E, Choi J, Jo Y, Kim JY, Jang YJ, Lee HM, Kim SY, Lee HJ, Cho K, Jung N, Hur EM, Jeong SJ, Moon C, Choe Y, Rhyu IJ, Kim H, Sun W. ACT-PRESTO: Rapid and consistent tissue clearing and labeling method for 3-dimensional (3D) imaging. Sci Rep 2016; 6:18631. [PMID: 26750588 PMCID: PMC4707495 DOI: 10.1038/srep18631] [Citation(s) in RCA: 143] [Impact Index Per Article: 17.9] [Reference Citation Analysis] [Abstract] [MESH Headings] [Track Full Text] [Download PDF] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Received: 09/08/2015] [Accepted: 11/23/2015] [Indexed: 12/20/2022] Open
Abstract
Understanding the structural organization of organs and organisms at the cellular level is a fundamental challenge in biology. This task has been approached by reconstructing three-dimensional structure from images taken from serially sectioned tissues, which is not only labor-intensive and time-consuming but also error-prone. Recent advances in tissue clearing techniques allow visualization of cellular structures and neural networks inside of unsectioned whole tissues or the entire body. However, currently available protocols require long process times. Here, we present the rapid and highly reproducible ACT-PRESTO (active clarity technique-pressure related efficient and stable transfer of macromolecules into organs) method that clears tissues or the whole body within 1 day while preserving tissue architecture and protein-based signals derived from endogenous fluorescent proteins. Moreover, ACT-PRESTO is compatible with conventional immunolabeling methods and expedites antibody penetration into thick specimens by applying pressure. The speed and consistency of this method will allow high-content mapping and analysis of normal and pathological features in intact organs and bodies.
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Affiliation(s)
- Eunsoo Lee
- Department of Anatomy and Division of Brain Korea 21 Plus Program for Biomedical Science, Korea University College of Medicine, Anam-dong, Seongbuk-gu, Seoul 136-705, Korea
| | - Jungyoon Choi
- Department of Anatomy and Division of Brain Korea 21 Plus Program for Biomedical Science, Korea University College of Medicine, Anam-dong, Seongbuk-gu, Seoul 136-705, Korea
| | - Youhwa Jo
- Department of Anatomy and Division of Brain Korea 21 Plus Program for Biomedical Science, Korea University College of Medicine, Anam-dong, Seongbuk-gu, Seoul 136-705, Korea
| | - Joo Yeon Kim
- Department of Anatomy and Division of Brain Korea 21 Plus Program for Biomedical Science, Korea University College of Medicine, Anam-dong, Seongbuk-gu, Seoul 136-705, Korea
| | - Yu Jin Jang
- Department of Neural Development and Disease, Korea Brain Research Institute, 701-300 Daegu, Korea
| | - Hye Myeong Lee
- Department of Neural Development and Disease, Korea Brain Research Institute, 701-300 Daegu, Korea
| | - So Yeun Kim
- Department of Brain & Cognitive Sciences, Graduate School, Daegu Gyeungbuk Institute of Science and Technology (DGIST), Daegu, Korea
| | - Ho-Jae Lee
- Logos Biosystems, Inc. Anyang-Si, Gyunggi-Do, 431-755, Republic of Korea
| | - Keunchang Cho
- Logos Biosystems, Inc. Anyang-Si, Gyunggi-Do, 431-755, Republic of Korea
| | - Neoncheol Jung
- Logos Biosystems, Inc. Anyang-Si, Gyunggi-Do, 431-755, Republic of Korea
| | - Eun Mi Hur
- Center for Neuroscience, Brain Science Institute, Korea Institute of Science and Technology, Seoul, Korea
- Department of Neuroscience, Korea University of Science and Technology (UST), Daejeon, Korea
| | - Sung Jin Jeong
- Department of Neural Development and Disease, Korea Brain Research Institute, 701-300 Daegu, Korea
| | - Cheil Moon
- Department of Brain & Cognitive Sciences, Graduate School, Daegu Gyeungbuk Institute of Science and Technology (DGIST), Daegu, Korea
| | - Youngshik Choe
- Department of Neural Development and Disease, Korea Brain Research Institute, 701-300 Daegu, Korea
| | - Im Joo Rhyu
- Department of Anatomy and Division of Brain Korea 21 Plus Program for Biomedical Science, Korea University College of Medicine, Anam-dong, Seongbuk-gu, Seoul 136-705, Korea
| | - Hyun Kim
- Department of Anatomy and Division of Brain Korea 21 Plus Program for Biomedical Science, Korea University College of Medicine, Anam-dong, Seongbuk-gu, Seoul 136-705, Korea
| | - Woong Sun
- Department of Anatomy and Division of Brain Korea 21 Plus Program for Biomedical Science, Korea University College of Medicine, Anam-dong, Seongbuk-gu, Seoul 136-705, Korea
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32
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Susaki E, Ueda H. Whole-body and Whole-Organ Clearing and Imaging Techniques with Single-Cell Resolution: Toward Organism-Level Systems Biology in Mammals. Cell Chem Biol 2016; 23:137-157. [DOI: 10.1016/j.chembiol.2015.11.009] [Citation(s) in RCA: 221] [Impact Index Per Article: 27.6] [Reference Citation Analysis] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Received: 11/03/2015] [Revised: 11/20/2015] [Accepted: 11/20/2015] [Indexed: 12/29/2022]
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