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Kurz B, Lange T, Voelker M, Hart ML, Rolauffs B. Articular Cartilage-From Basic Science Structural Imaging to Non-Invasive Clinical Quantitative Molecular Functional Information for AI Classification and Prediction. Int J Mol Sci 2023; 24:14974. [PMID: 37834422 PMCID: PMC10573252 DOI: 10.3390/ijms241914974] [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: 09/08/2023] [Revised: 09/25/2023] [Accepted: 09/27/2023] [Indexed: 10/15/2023] Open
Abstract
This review presents the changes that the imaging of articular cartilage has undergone throughout the last decades. It highlights that the expectation is no longer to image the structure and associated functions of articular cartilage but, instead, to devise methods for generating non-invasive, function-depicting images with quantitative information that is useful for detecting the early, pre-clinical stage of diseases such as primary or post-traumatic osteoarthritis (OA/PTOA). In this context, this review summarizes (a) the structure and function of articular cartilage as a molecular imaging target, (b) quantitative MRI for non-invasive assessment of articular cartilage composition, microstructure, and function with the current state of medical diagnostic imaging, (c), non-destructive imaging methods, (c) non-destructive quantitative articular cartilage live-imaging methods, (d) artificial intelligence (AI) classification of degeneration and prediction of OA progression, and (e) our contribution to this field, which is an AI-supported, non-destructive quantitative optical biopsy for early disease detection that operates on a digital tissue architectural fingerprint. Collectively, this review shows that articular cartilage imaging has undergone profound changes in the purpose and expectations for which cartilage imaging is used; the image is becoming an AI-usable biomarker with non-invasive quantitative functional information. This may aid in the development of translational diagnostic applications and preventive or early therapeutic interventions that are yet beyond our reach.
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Affiliation(s)
- Bodo Kurz
- Department of Anatomy, Christian-Albrechts-University, Otto-Hahn-Platz 8, 24118 Kiel, Germany
| | - Thomas Lange
- Medical Physics Department of Radiology, Faculty of Medicine, Medical Center—Albert-Ludwigs-University of Freiburg, 79085 Freiburg im Breisgau, Germany;
| | - Marita Voelker
- G.E.R.N. Research Center for Tissue Replacement, Regeneration & Neogenesis, Department of Orthopedics and Trauma Surgery, Faculty of Medicine, Medical Center—Albert-Ludwigs-University of Freiburg, 79085 Freiburg im Breisgau, Germany; (M.V.); (M.L.H.)
| | - Melanie L. Hart
- G.E.R.N. Research Center for Tissue Replacement, Regeneration & Neogenesis, Department of Orthopedics and Trauma Surgery, Faculty of Medicine, Medical Center—Albert-Ludwigs-University of Freiburg, 79085 Freiburg im Breisgau, Germany; (M.V.); (M.L.H.)
| | - Bernd Rolauffs
- G.E.R.N. Research Center for Tissue Replacement, Regeneration & Neogenesis, Department of Orthopedics and Trauma Surgery, Faculty of Medicine, Medical Center—Albert-Ludwigs-University of Freiburg, 79085 Freiburg im Breisgau, Germany; (M.V.); (M.L.H.)
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2
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Liu K, Lei Y, Li D. Simultaneous 3D Construction and Imaging of Plant Cells Using Plasmonic Nanoprobe-Assisted Multimodal Nonlinear Optical Microscopy. NANOMATERIALS (BASEL, SWITZERLAND) 2023; 13:2626. [PMID: 37836267 PMCID: PMC10574158 DOI: 10.3390/nano13192626] [Citation(s) in RCA: 0] [Impact Index Per Article: 0] [Reference Citation Analysis] [Abstract] [Key Words] [Grants] [Track Full Text] [Subscribe] [Scholar Register] [Received: 08/22/2023] [Revised: 09/10/2023] [Accepted: 09/21/2023] [Indexed: 10/15/2023]
Abstract
Nonlinear optical (NLO) imaging has emerged as a promising plant cell imaging technique due to its large optical penetration, inherent 3D spatial resolution, and reduced photodamage; exogenous nanoprobes are usually needed for nonsignal target cell analysis. Here, we report in vivo, simultaneous 3D labeling and imaging of potato cell structures using plasmonic nanoprobe-assisted multimodal NLO microscopy. Experimental results show that the complete cell structure can be imaged via the combination of second-harmonic generation (SHG) and two-photon luminescence (TPL) when noble metal silver or gold ions are added. In contrast, without the noble metal ion solution, no NLO signals from the cell wall were acquired. The mechanism can be attributed to noble metal nanoprobes with strong nonlinear optical responses formed along the cell walls via a femtosecond laser scan. During the SHG-TPL imaging process, noble metal ions that crossed the cell wall were rapidly reduced to plasmonic nanoparticles with the fs laser and selectively anchored onto both sides of the cell wall, thereby leading to simultaneous 3D labeling and imaging of the potato cells. Compared with the traditional labeling technique that needs in vitro nanoprobe fabrication and cell labeling, our approach allows for one-step, in vivo labeling of plant cells, thus providing a rapid, cost-effective method for cellular structure construction and imaging.
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Affiliation(s)
- Kun Liu
- School of Optoelectronic Engineering and Instrumentation Science, Dalian University of Technology, Dalian 116024, China
| | - Yutian Lei
- Department of Civil Engineering, University of Nebraska-Lincoln, Lincoln, NE 68588, USA
| | - Dawei Li
- School of Optoelectronic Engineering and Instrumentation Science, Dalian University of Technology, Dalian 116024, China
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3
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Fernández-Galiana Á, Bibikova O, Vilms Pedersen S, Stevens MM. Fundamentals and Applications of Raman-Based Techniques for the Design and Development of Active Biomedical Materials. ADVANCED MATERIALS (DEERFIELD BEACH, FLA.) 2023:e2210807. [PMID: 37001970 DOI: 10.1002/adma.202210807] [Citation(s) in RCA: 0] [Impact Index Per Article: 0] [Reference Citation Analysis] [Abstract] [Key Words] [Grants] [Track Full Text] [Subscribe] [Scholar Register] [Received: 11/21/2022] [Revised: 03/03/2023] [Indexed: 06/19/2023]
Abstract
Raman spectroscopy is an analytical method based on light-matter interactions that can interrogate the vibrational modes of matter and provide representative molecular fingerprints. Mediated by its label-free, non-invasive nature, and high molecular specificity, Raman-based techniques have become ubiquitous tools for in situ characterization of materials. This review comprehensively describes the theoretical and practical background of Raman spectroscopy and its advanced variants. The numerous facets of material characterization that Raman scattering can reveal, including biomolecular identification, solid-to-solid phase transitions, and spatial mapping of biomolecular species in bioactive materials, are highlighted. The review illustrates the potential of these techniques in the context of active biomedical material design and development by highlighting representative studies from the literature. These studies cover the use of Raman spectroscopy for the characterization of both natural and synthetic biomaterials, including engineered tissue constructs, biopolymer systems, ceramics, and nanoparticle formulations, among others. To increase the accessibility and adoption of these techniques, the present review also provides the reader with practical recommendations on the integration of Raman techniques into the experimental laboratory toolbox. Finally, perspectives on how recent developments in plasmon- and coherently-enhanced Raman spectroscopy can propel Raman from underutilized to critical for biomaterial development are provided.
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Affiliation(s)
- Álvaro Fernández-Galiana
- Department of Materials, Department of Bioengineering, Imperial College London, SW7 2AZ, London, UK
| | - Olga Bibikova
- Department of Materials, Department of Bioengineering, Imperial College London, SW7 2AZ, London, UK
| | - Simon Vilms Pedersen
- Department of Materials, Department of Bioengineering, Imperial College London, SW7 2AZ, London, UK
| | - Molly M Stevens
- Department of Materials, Department of Bioengineering, Imperial College London, SW7 2AZ, London, UK
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4
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Halsey G, Sinha D, Dhital S, Wang X, Vyavahare N. Role of elastic fiber degradation in disease pathogenesis. Biochim Biophys Acta Mol Basis Dis 2023; 1869:166706. [PMID: 37001705 DOI: 10.1016/j.bbadis.2023.166706] [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: 10/28/2022] [Revised: 03/22/2023] [Accepted: 03/23/2023] [Indexed: 03/31/2023]
Abstract
Elastin is a crucial extracellular matrix protein that provides structural integrity to tissues. Crosslinked elastin and associated microfibrils, named elastic fiber, contribute to biomechanics by providing the elasticity required for proper function. During aging and disease, elastic fiber can be progressively degraded and since there is little elastin synthesis in adults, degraded elastic fiber is not regenerated. There is substantial evidence linking loss or damage of elastic fibers to the clinical manifestation and pathogenesis of a variety of diseases. Disruption of elastic fiber networks by hereditary mutations, aging, or pathogenic stimuli results in systemic ailments associated with the production of elastin degradation products, inflammatory responses, and abnormal physiology. Due to its longevity, unique mechanical properties, and widespread distribution in the body, elastic fiber plays a central role in homeostasis of various physiological systems. While pathogenesis related to elastic fiber degradation has been more thoroughly studied in elastic fiber rich tissues such as the vasculature and the lungs, even tissues containing relatively small quantities of elastic fibers such as the eyes or joints may be severely impacted by elastin degradation. Elastic fiber degradation is a common observation in certain hereditary, age, and specific risk factor exposure induced diseases representing a converging point of pathological clinical phenotypes which may also help explain the appearance of co-morbidities. In this review, we will first cover the role of elastic fiber degradation in the manifestation of hereditary diseases then individually explore the structural role and degradation effects of elastic fibers in various tissues and organ systems. Overall, stabilizing elastic fiber structures and repairing lost elastin may be effective strategies to reverse the effects of these diseases.
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Affiliation(s)
- Gregory Halsey
- Department of Bioengineering, Clemson University, SC 29634, United States of America
| | - Dipasha Sinha
- Department of Bioengineering, Clemson University, SC 29634, United States of America
| | - Saphala Dhital
- Department of Bioengineering, Clemson University, SC 29634, United States of America
| | - Xiaoying Wang
- Department of Bioengineering, Clemson University, SC 29634, United States of America
| | - Naren Vyavahare
- Department of Bioengineering, Clemson University, SC 29634, United States of America.
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Zoltan S, Jonathan C, Jeremy M, Marie-Laure P, Kevin J, Claude C, Le Flahec A, Claire LB, Charbel M, Aymeric R, Bardet SM. A novel histological occlusion classification for coiled aneurysms based on multiphoton microscopy. Interv Neuroradiol 2023:15910199231157926. [PMID: 36803150 DOI: 10.1177/15910199231157926] [Citation(s) in RCA: 0] [Impact Index Per Article: 0] [Reference Citation Analysis] [Abstract] [Key Words] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Indexed: 02/22/2023] Open
Abstract
OBJECTIVE Intracranial aneurysm (IA) coiling remains the most commonly used endovascular approach for ruptured and unruptured IA, and recanalization is a common drawback that impairs treatment success. Angiographic occlusion and aneurysm healing are not synonymous, and histological evaluation of embolized aneurysms remains a challenge. We propose here an experimental study of coil embolization in animal models by multiphoton microscopy (MPM) in comparison with conventional histological staining. The purpose of his work is to analyze coil healing process using histological sections of aneurysms. METHODS Based on a rabbit elastase model, 27 aneurysms were fixed, embedded in resin, and cut in thin histological sections 1 month after coils implantation and after angiographic control. Hematoxylin and eosin (H&S) staining were realized. Non-stained adjacent slices were imaged for multiphoton excited autofluorescence (AF) and second-harmonic generation (SHG) to construct three-dimensional (3D) projections of sequentially and axially acquired images. RESULTS The contrast provided by the combination of these two imaging modalities can be used to distinguish five levels of aneurysm healing, based on a combination of thrombus evolution and increased extracellular matrix (ECM) deposit. CONCLUSION RDPC:\Users\SHAHUL\RDP6|We have established a novel histological scale from a rabbit elastase aneurysm model after coiling with a classification of five different stages thanks to nonlinear microscopy. This classification is an actualized tool in order to obtain a more precise evaluation of occlusion device efficacy in the scope of new innovative microscopy for research.
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Affiliation(s)
- Szatmary Zoltan
- Neuroradiology Department, 27025Limoges University, Dupuytren Hospital, Limoges, France
- XLIM UMR CNRS 7252 Limoges, Aquitaine, France
| | - Cortese Jonathan
- XLIM UMR CNRS 7252 Limoges, Aquitaine, France
- Neuroradiology Department, Hôpital Bicêtre Interventional, Le Kremlin Bicêtre, Ile-de-France, France
| | - Mounier Jeremy
- XLIM UMR CNRS 7252 Limoges, Aquitaine, France
- 27025Medical Faculty, Limoges University, Limoges, France
| | | | - Janot Kevin
- XLIM UMR CNRS 7252 Limoges, Aquitaine, France
- Neuroradiology Department, University Hospital of Tours, Tours, France
| | - Couquet Claude
- 27025Medical Faculty, Limoges University, Limoges, France
| | | | | | - Mounayer Charbel
- Neuroradiology Department, 27025Limoges University, Dupuytren Hospital, Limoges, France
- XLIM UMR CNRS 7252 Limoges, Aquitaine, France
| | - Rouchaud Aymeric
- Neuroradiology Department, 27025Limoges University, Dupuytren Hospital, Limoges, France
- XLIM UMR CNRS 7252 Limoges, Aquitaine, France
| | - Sylvia M Bardet
- XLIM UMR CNRS 7252 Limoges, Aquitaine, France
- 27025Medical Faculty, Limoges University, Limoges, France
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6
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de Guzman RC, Meer AS, Mathews AA, Israel AR, Moses MT, Sams CM, Deegan DB. Reduced fibrous capsule elastic fibers from biologic ECM-enveloped CIEDs in minipigs, supported with a novel compression mechanics model. Biomed Mater Eng 2022:BME221488. [PMID: 36617774 DOI: 10.3233/bme-221488] [Citation(s) in RCA: 0] [Impact Index Per Article: 0] [Reference Citation Analysis] [Abstract] [Key Words] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Indexed: 01/05/2023]
Abstract
BACKGROUND Fibrous capsules (Fb) in response to cardiovascular implantable electronic devices (CIEDs), including a pacemaker (P) system, can produce patient discomfort and difficulties in revision surgery due partially to their increased compressive strength, previously linked to elevated tissue fibers. OBJECTIVE A preliminary study to quantify structural proteins, determine if biologic extracellular matrix-enveloped CIEDs (PECM) caused differential Fb properties, and to implement a realistic mechanical model. METHODS Retrieved Fb (-P and -PECM) from minipigs were subjected to biomechanical (shear oscillation and uniaxial compression) and histological (collagen I and elastin) analyses. RESULTS Fb-PECM showed significant decreases compared to Fb-P in: low strain-loss modulus (390 vs. 541 Pa) across angular frequencies, high strain-compressive elastic modulus (1043 vs. 2042 kPa), and elastic fiber content (1.92 vs. 3.15 μg/mg tissue). Decreases in elastin were particularly noted closer to the implant's surface (Fb-PECM = 71% vs. Fb-P = 143% relative to dermal elastin at mid-tangential sections) and verified with a solid mechanics hyperelasticity with direction-dependent fiber viscoelasticity compression simulation (r2 ≥ 98.9%). CONCLUSIONS The biologic envelope composed of decellularized porcine small intestine submucosa ECM for CIEDs promoted fibrous tissues with less elastic fibers. Novel compression modeling analyses directly correlated this singular reduction to more desirable subcutaneous tissue mechanics.
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Affiliation(s)
- Roche C de Guzman
- Bioengineering Program, Department of Engineering, Hofstra University, Hempstead, NY, USA
| | - Allison S Meer
- Bioengineering Program, Department of Engineering, Hofstra University, Hempstead, NY, USA.,Department of Biology, Hofstra University, Hempstead, NY, USA
| | - Aidan A Mathews
- Bioengineering Program, Department of Engineering, Hofstra University, Hempstead, NY, USA.,Department of Biology, Hofstra University, Hempstead, NY, USA
| | - Atara R Israel
- Bioengineering Program, Department of Engineering, Hofstra University, Hempstead, NY, USA
| | - Michael T Moses
- Bioengineering Program, Department of Engineering, Hofstra University, Hempstead, NY, USA
| | - Clarence M Sams
- Bioengineering Program, Department of Engineering, Hofstra University, Hempstead, NY, USA
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Al-Maslamani NA, Oldershaw R, Tew S, Curran J, D’Hooghe P, Yamamoto K, Horn HF. Chondrocyte De-Differentiation: Biophysical Cues to Nuclear Alterations. Cells 2022; 11:cells11244011. [PMID: 36552775 PMCID: PMC9777101 DOI: 10.3390/cells11244011] [Citation(s) in RCA: 2] [Impact Index Per Article: 1.0] [Reference Citation Analysis] [Abstract] [Key Words] [MESH Headings] [Grants] [Track Full Text] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Received: 10/20/2022] [Revised: 11/29/2022] [Accepted: 12/05/2022] [Indexed: 12/14/2022] Open
Abstract
Autologous chondrocyte implantation (ACI) is a cell therapy to repair cartilage defects. In ACI a biopsy is taken from a non-load bearing area of the knee and expanded in-vitro. The expansion process provides the benefit of generating a large number of cells required for implantation; however, during the expansion these cells de-differentiate and lose their chondrocyte phenotype. In this review we focus on examining the de-differentiation phenotype from a mechanobiology and biophysical perspective, highlighting some of the nuclear mechanics and chromatin changes in chondrocytes seen during the expansion process and how this relates to the gene expression profile. We propose that manipulating chondrocyte nuclear architecture and chromatin organization will highlight mechanisms that will help to preserve the chondrocyte phenotype.
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Affiliation(s)
- Noor A. Al-Maslamani
- Department of Musculoskeletal and Ageing Science, Institute of Life Course and Medical Sciences, University of Liverpool, Liverpool L7 8TX, UK
- Correspondence:
| | - Rachel Oldershaw
- Department of Musculoskeletal and Ageing Science, Institute of Life Course and Medical Sciences, University of Liverpool, Liverpool L7 8TX, UK
| | - Simon Tew
- Department of Musculoskeletal and Ageing Science, Institute of Life Course and Medical Sciences, University of Liverpool, Liverpool L7 8TX, UK
| | - Jude Curran
- Department of Mechanical, Materials and Aerospace Engineering, School of Engineering, University of Liverpool, Liverpool L69 3GH, UK
| | - Pieter D’Hooghe
- Department of Orthopaedic Surgery, Aspetar Orthopaedic and Sports Medicine Hospital, Doha P.O. Box 29222, Qatar
| | - Kazuhiro Yamamoto
- Department of Musculoskeletal and Ageing Science, Institute of Life Course and Medical Sciences, University of Liverpool, Liverpool L7 8TX, UK
| | - Henning F. Horn
- College of Health and Life Sciences, Hamad Bin Khalifa University, Doha P.O. Box 34110, Qatar
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8
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Boos MA, Lamandé SR, Stok KS. Multiscale Strain Transfer in Cartilage. Front Cell Dev Biol 2022; 10:795522. [PMID: 35186920 PMCID: PMC8855033 DOI: 10.3389/fcell.2022.795522] [Citation(s) in RCA: 0] [Impact Index Per Article: 0] [Reference Citation Analysis] [Abstract] [Track Full Text] [Download PDF] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Received: 10/15/2021] [Accepted: 01/19/2022] [Indexed: 11/30/2022] Open
Abstract
The transfer of stress and strain signals between the extracellular matrix (ECM) and cells is crucial for biochemical and biomechanical cues that are required for tissue morphogenesis, differentiation, growth, and homeostasis. In cartilage tissue, the heterogeneity in spatial variation of ECM molecules leads to a depth-dependent non-uniform strain transfer and alters the magnitude of forces sensed by cells in articular and fibrocartilage, influencing chondrocyte metabolism and biochemical response. It is not fully established how these nonuniform forces ultimately influence cartilage health, maintenance, and integrity. To comprehend tissue remodelling in health and disease, it is fundamental to investigate how these forces, the ECM, and cells interrelate. However, not much is known about the relationship between applied mechanical stimulus and resulting spatial variations in magnitude and sense of mechanical stimuli within the chondrocyte’s microenvironment. Investigating multiscale strain transfer and hierarchical structure-function relationships in cartilage is key to unravelling how cells receive signals and how they are transformed into biosynthetic responses. Therefore, this article first reviews different cartilage types and chondrocyte mechanosensing. Following this, multiscale strain transfer through cartilage tissue and the involvement of individual ECM components are discussed. Finally, insights to further understand multiscale strain transfer in cartilage are outlined.
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Affiliation(s)
- Manuela A. Boos
- Department of Biomedical Engineering, The University of Melbourne, Parkville, VIC, Australia
| | - Shireen R. Lamandé
- Musculoskeletal Research, Murdoch Children’s Research Institute, Parkville, VIC, Australia
- Department of Paediatrics, The University of Melbourne, Parkville, VIC, Australia
| | - Kathryn S. Stok
- Department of Biomedical Engineering, The University of Melbourne, Parkville, VIC, Australia
- *Correspondence: Kathryn S. Stok,
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9
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Sherlock B, Chen J, Mansfield J, Green E, Winlove C. Biophotonic tools for probing extracellular matrix mechanics. Matrix Biol Plus 2021; 12:100093. [PMID: 34934939 PMCID: PMC8661043 DOI: 10.1016/j.mbplus.2021.100093] [Citation(s) in RCA: 1] [Impact Index Per Article: 0.3] [Reference Citation Analysis] [Abstract] [Key Words] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Received: 07/30/2021] [Revised: 11/07/2021] [Accepted: 11/11/2021] [Indexed: 12/11/2022] Open
Abstract
The complex, hierarchical and heterogeneous biomechanics of the extracellular matrix (ECM) are central to the health of multicellular organisms. Characterising the distribution, dynamics and above all else origins of ECM biomechanics are challenges that have captivated researchers for decades. Recently, a suite of biophotonics techniques have emerged as powerful new tools to investigate ECM biomechanics. In this mini-review, we discuss how the non-destructive, sub-micron resolution imaging capabilities of Raman spectroscopy and nonlinear microscopy are being used to interrogate the biomechanics of thick, living tissues. These high speed, label-free techniques are implemented during mechanical testing, providing unprecedented insight into the compositional and structural response of the ECM to changes in the mechanical environment.
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Affiliation(s)
- B.E. Sherlock
- College of Medicine and Health, University of Exeter, Exeter EX1 2LU, United Kingdom
| | - J. Chen
- College of Engineering, Mathematical and Physical Sciences, University of Exeter, Exeter EX4 4QF, United Kingdom
| | - J.C. Mansfield
- College of Engineering, Mathematical and Physical Sciences, University of Exeter, Exeter EX4 4QF, United Kingdom
| | - E. Green
- College of Engineering, Mathematical and Physical Sciences, University of Exeter, Exeter EX4 4QF, United Kingdom
| | - C.P. Winlove
- College of Engineering, Mathematical and Physical Sciences, University of Exeter, Exeter EX4 4QF, United Kingdom
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10
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Wu JP, Yang X, Wang Y, Swift B, Adamson R, Zheng Y, Zhang R, Zhong W, Chen F. High Resolution and Labeling Free Studying the 3D Microstructure of the Pars Tensa-Annulus Unit of Mice. Front Cell Dev Biol 2021; 9:720383. [PMID: 34692679 PMCID: PMC8532514 DOI: 10.3389/fcell.2021.720383] [Citation(s) in RCA: 2] [Impact Index Per Article: 0.7] [Reference Citation Analysis] [Abstract] [Key Words] [Track Full Text] [Download PDF] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Received: 06/04/2021] [Accepted: 08/13/2021] [Indexed: 11/21/2022] Open
Abstract
Hearing loss is a serious illness affecting people’s normal life enormously. The acoustic properties of a tympanic membrane play an important role in hearing, and highly depend on its geometry, composition, microstructure and connection to the surrounding annulus. While the conical geometry of the tympanic membrane is critical to the sound propagation in the auditory system, it presents significant challenges to the study of the 3D microstructure of the tympanic membrane using traditional 2D imaging techniques. To date, most of our knowledge about the 3D microstructure and composition of tympanic membranes is built from 2D microscopic studies, which precludes an accurate understanding of the 3D microstructure, acoustic behaviors and biology of the tissue. Although the tympanic membrane has been reported to contain elastic fibers, the morphological characteristic of the elastic fibers and the spatial arrangement of the elastic fibers with the predominant collagen fibers have not been shown in images. We have developed a 3D imaging technique for the three-dimensional examination of the microstructure of the full thickness of the tympanic membranes in mice without requiring tissue dehydration and stain. We have also used this imaging technique to study the 3D arrangement of the collagen and elastic fibrillar network with the capillaries and cells in the pars tensa-annulus unit at a status close to the native. The most striking findings in the study are the discovery of the 3D form of the elastic and collagen network, and the close spatial relationships between the elastic fibers and the elongated fibroblasts in the tympanic membranes. The 3D imaging technique has enabled to show the 3D waveform contour of the collagen and elastic scaffold in the conical tympanic membrane. Given the close relationship among the acoustic properties, composition, 3D microstructure and geometry of tympanic membranes, the findings may advance the understanding of the structure—acoustic functionality of the tympanic membrane. The knowledge will also be very helpful in the development of advanced cellular therapeutic technologies and 3D printing techniques to restore damaged tympanic membranes to a status close to the native.
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Affiliation(s)
- Jian-Ping Wu
- Academy of Advanced Interdisciplinary Studies, Southern University of Science and Technology, Shenzhen, China.,Department of Biomedical Engineering, Southern University of Science and Technology, Shenzhen, China
| | - Xiaojie Yang
- Department of Biomedical Engineering, Southern University of Science and Technology, Shenzhen, China
| | - Yilin Wang
- Core Research Facilities, Southern University of Science and Technology, Shenzhen, China
| | - Ben Swift
- College of Computing, Australian National University, Canberra, ACT, Australia
| | - Robert Adamson
- School of Biomedical Engineering, Electrical and Computer Engineering, Dalhousie University, Halifax, NS, Canada
| | - Yongchang Zheng
- Peking Union Medical College Hospital, Chinese Academy of Medical Sciences and Peking Union Medical College, Beijing, China
| | - Rongli Zhang
- Guangdong Provincial People's Hospital, Guangdong Academy of Medical Science, School of Medicine, South China University of Technology, Guangzhou, China
| | - Wen Zhong
- School of Mechanical Engineering and Automation, Xihua University, Chengdu, China
| | - Fangyi Chen
- Department of Biomedical Engineering, Southern University of Science and Technology, Shenzhen, China.,Department of Biology, Brain Research Centre, Southern University of Science and Technology, Shenzhen, China
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11
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Lin W, Klein J. Recent Progress in Cartilage Lubrication. ADVANCED MATERIALS (DEERFIELD BEACH, FLA.) 2021; 33:e2005513. [PMID: 33759245 DOI: 10.1002/adma.202005513] [Citation(s) in RCA: 136] [Impact Index Per Article: 45.3] [Reference Citation Analysis] [Abstract] [Key Words] [MESH Headings] [Grants] [Track Full Text] [Subscribe] [Scholar Register] [Received: 08/13/2020] [Revised: 11/23/2020] [Indexed: 05/18/2023]
Abstract
Healthy articular cartilage, covering the ends of bones in major joints such as hips and knees, presents the most efficiently-lubricated surface known in nature, with friction coefficients as low as 0.001 up to physiologically high pressures. Such low friction is indeed essential for its well-being. It minimizes wear-and-tear and hence the cartilage degradation associated with osteoarthritis, the most common joint disease, and, by reducing shear stress on the mechanotransductive, cartilage-embedded chondrocytes (the only cell type in the cartilage), it regulates their function to maintain homeostasis. Understanding the origins of such low friction of the articular cartilage, therefore, is of major importance in order to alleviate disease symptoms, and slow or even reverse its breakdown. This progress report considers the relation between frictional behavior and the cellular mechanical environment in the cartilage, then reviews the mechanism of lubrication in the joints, in particular focusing on boundary lubrication. Following recent advances based on hydration lubrication, a proposed synergy between different molecular components of the synovial joints, acting together in enabling the low friction, has been proposed. Additionally, recent development of natural and bio-inspired lubricants is reviewed.
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Affiliation(s)
- Weifeng Lin
- Department of Materials and Interfaces, Weizmann Institute of Science, Rehovot, 76100, Israel
| | - Jacob Klein
- Department of Materials and Interfaces, Weizmann Institute of Science, Rehovot, 76100, Israel
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12
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Wang JY, Mansfield JC, Brasselet S, Vergari C, Meakin JR, Winlove CP. Micro-mechanical damage of needle puncture on bovine annulus fibrosus fibrils studied using polarization-resolved Second Harmonic Generation(P-SHG) microscopy. J Mech Behav Biomed Mater 2021; 118:104458. [PMID: 33761373 DOI: 10.1016/j.jmbbm.2021.104458] [Citation(s) in RCA: 4] [Impact Index Per Article: 1.3] [Reference Citation Analysis] [Abstract] [Key Words] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Received: 07/15/2020] [Revised: 02/28/2021] [Accepted: 03/10/2021] [Indexed: 11/24/2022]
Abstract
Needle injection has been widely used in spinal therapeutic or diagnostic processes, such as discography. The use of needles has been suspected in causing mild disc degeneration which can lead to long-term back pain. However, the localised microscopic damage caused by needles has not been well studied. The local progressive damage on a microscopic level caused by needle punctures on the surface of bovine annulus fibrosus was investigated. Four different sizes of needle were used for the puncture and twenty-nine bovine intervertebral discs were studied. Polarization-resolved second harmonic generation and fluorescent microscopy were used to study the local microscopic structural changes in collagen and cell nuclei due to needle damage. Repeated 70 cyclic loadings at ±5% of axial strain were applied after the needle puncture in order to assess progressive damage caused by the needle. Puncture damage on annulus fibrosus were observed either collagen fibre bundles being pushed aside, being cut through or combination of both with part being lift or pushed in. The progressive damage was found less relevant to the needle size and more progressive damage was only observed using the larger needle. Two distinct populations of collagen, in which one was relatively more organised than the other population, were observed especially after the puncture from skewed distribution of polarization-SHG analysis. Cell shape was found rounder near the puncture site where collagen fibres were damaged.
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Affiliation(s)
- J-Y Wang
- College of Engineering, Mathematics & Physical Sciences, Physics Building, Stocker Road, Exeter, EX4 4QL, UK.
| | - J C Mansfield
- College of Engineering, Mathematics & Physical Sciences, Physics Building, Stocker Road, Exeter, EX4 4QL, UK
| | - S Brasselet
- Aix Marseille Univ, CNRS, Centrale Marseille, Institut Fresnel, F-13013, Marseille, France
| | - C Vergari
- Arts et Métiers Institute of Technology, Université Sorbonne Paris Nord, IBHGC - Institut de Biomécanique Humaine Georges Charpak, HESAM Université, F-75013, Paris
| | - J R Meakin
- College of Engineering, Mathematics & Physical Sciences, Physics Building, Stocker Road, Exeter, EX4 4QL, UK
| | - C P Winlove
- College of Engineering, Mathematics & Physical Sciences, Physics Building, Stocker Road, Exeter, EX4 4QL, UK
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13
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Querido W, Kandel S, Pleshko N. Applications of Vibrational Spectroscopy for Analysis of Connective Tissues. Molecules 2021; 26:922. [PMID: 33572384 PMCID: PMC7916244 DOI: 10.3390/molecules26040922] [Citation(s) in RCA: 36] [Impact Index Per Article: 12.0] [Reference Citation Analysis] [Abstract] [Key Words] [MESH Headings] [Grants] [Track Full Text] [Download PDF] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Received: 12/31/2020] [Revised: 01/30/2021] [Accepted: 02/04/2021] [Indexed: 02/07/2023] Open
Abstract
Advances in vibrational spectroscopy have propelled new insights into the molecular composition and structure of biological tissues. In this review, we discuss common modalities and techniques of vibrational spectroscopy, and present key examples to illustrate how they have been applied to enrich the assessment of connective tissues. In particular, we focus on applications of Fourier transform infrared (FTIR), near infrared (NIR) and Raman spectroscopy to assess cartilage and bone properties. We present strengths and limitations of each approach and discuss how the combination of spectrometers with microscopes (hyperspectral imaging) and fiber optic probes have greatly advanced their biomedical applications. We show how these modalities may be used to evaluate virtually any type of sample (ex vivo, in situ or in vivo) and how "spectral fingerprints" can be interpreted to quantify outcomes related to tissue composition and quality. We highlight the unparalleled advantage of vibrational spectroscopy as a label-free and often nondestructive approach to assess properties of the extracellular matrix (ECM) associated with normal, developing, aging, pathological and treated tissues. We believe this review will assist readers not only in better understanding applications of FTIR, NIR and Raman spectroscopy, but also in implementing these approaches for their own research projects.
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Affiliation(s)
| | | | - Nancy Pleshko
- Department of Bioengineering, Temple University, Philadelphia, PA 19122, USA; (W.Q.); (S.K.)
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14
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Bardet SM, Cortese J, Blanc R, Mounayer C, Rouchaud A. Multiphoton microscopy for pre-clinical evaluation of flow-diverter stents for treating aneurysms. J Neuroradiol 2020; 48:200-206. [PMID: 32205257 DOI: 10.1016/j.neurad.2020.03.005] [Citation(s) in RCA: 1] [Impact Index Per Article: 0.3] [Reference Citation Analysis] [Abstract] [Key Words] [MESH Headings] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Received: 12/13/2019] [Revised: 03/09/2020] [Accepted: 03/10/2020] [Indexed: 12/17/2022]
Abstract
BACKGROUND Conventional histological analyses are the gold standard for the study of aneurysms and vascular pathologies in pre-clinical research. Over the past decade, in vivo and ex vivo imaging using multiphoton microscopy have emerged as powerful pre-clinical tools for detailed tissue analyses that can assess morphology, the extracellular matrix (ECM), cell density and vascularisation. Multiphoton microscopy allows for deeper tissue penetration with minor phototoxicity. OBJECTIVE The present study aimed to demonstrate the current status of multimodality imaging, including multiphoton microscopy, for detailed analyses of neo-endothelialisation and ECM evolution after flow-diverter stent (FDS) treatment in an experimental rabbit model of aneurysms. METHODS Multiphoton microscopy tools for assessing autofluorescence and second harmonic generation (SHG) signals from biological tissues were used to evaluate the endovascular treatment of intracranial aneurysms in an animal model of aneurysms (pig, rabbit). Results from multiphoton microscopy were compared to those from standard histology, electronic and bright field microscopy. CONCLUSIONS The present study describes novel evaluation modes based on multiphoton microscopy for visualising tissue morphology (e.g., collagen, elastin, and cells) to qualify and quantify the extent of neo-intimal formation of covered arteries and device integration into the arterial wall using a rabbit model of intracranial aneurysms treated with FDS.
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Affiliation(s)
- Sylvia M Bardet
- University of Limoges, 123, avenue Albert-Thomas, XLIM UMR CNRS 7252, 87060 Limoges, France.
| | - Jonathan Cortese
- Bichat University Hospital, INSERM U1148-LVTS, Paris, France; Bicetre Hospital, Department of Interventional Neuroradiology, Paris, France
| | - Raphaël Blanc
- Department of Interventional Neuroradiology, Fondation Ophtalmologique Adolphe-de-Rothschild, Paris, France
| | - Charbel Mounayer
- University of Limoges, 123, avenue Albert-Thomas, XLIM UMR CNRS 7252, 87060 Limoges, France; University Hospital, Department of Interventional Neuroradiology, Limoges, France
| | - Aymeric Rouchaud
- University of Limoges, 123, avenue Albert-Thomas, XLIM UMR CNRS 7252, 87060 Limoges, France; University Hospital, Department of Interventional Neuroradiology, Limoges, France.
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15
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Shoaib T, Yuh C, Wimmer MA, Schmid TM, Espinosa-Marzal RM. Nanoscale insight into the degradation mechanisms of the cartilage articulating surface preceding OA. Biomater Sci 2020; 8:3944-3955. [DOI: 10.1039/d0bm00496k] [Citation(s) in RCA: 9] [Impact Index Per Article: 2.3] [Reference Citation Analysis] [Abstract] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Indexed: 01/27/2023]
Abstract
Osteoarthritis (OA) is a degenerative disease and leading cause of disability globally. We report the a fundamental study of the mechanisms underlying deterioration of hydrated cartilage in the presence of elevated calcium content preceding OA.
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Affiliation(s)
- Tooba Shoaib
- Materials Science and Engineering
- University of Illinois at Urbana-Champaign
- Urbana
- USA
| | - Catherine Yuh
- Department of Orthopedics
- Rush University Medical Center
- Chicago
- USA
| | - Markus A. Wimmer
- Department of Orthopedics
- Rush University Medical Center
- Chicago
- USA
| | - Thomas M. Schmid
- Department of Orthopedics
- Rush University Medical Center
- Chicago
- USA
| | - Rosa M. Espinosa-Marzal
- Materials Science and Engineering
- University of Illinois at Urbana-Champaign
- Urbana
- USA
- Civil and Environmental Engineering Department
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16
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Maturation of the Meniscal Collagen Structure Revealed by Polarization-Resolved and Directional Second Harmonic Generation Microscopy. Sci Rep 2019; 9:18448. [PMID: 31804577 PMCID: PMC6895152 DOI: 10.1038/s41598-019-54942-0] [Citation(s) in RCA: 14] [Impact Index Per Article: 2.8] [Reference Citation Analysis] [Abstract] [Track Full Text] [Download PDF] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Received: 07/11/2019] [Accepted: 11/12/2019] [Indexed: 11/08/2022] Open
Abstract
We report Polarization-resolved Second Harmonic Generation (P-SHG) and directional SHG (forward and backward, F/B) measurements of equine foetal and adult collagen in meniscus, over large field-of-views using sample-scanning. Large differences of collagen structure and fibril orientation with maturation are revealed, validating the potential for this novel methodology to track such changes in meniscal structure. The foetal menisci had a non-organized and more random collagen fibrillar structure when compared with adult using P-SHG. For the latter, clusters of homogeneous fibril orientation (inter-fibrillar areas) were revealed, separated by thick fibers. F/B SHG showed numerous different features in adults notably, in thick fibers compared to interfibrillar areas, unlike foetal menisci that showed similar patterns for both directions. This work confirms previous studies and improves the understanding of meniscal collagen structure and its maturation, and makes F/B and P-SHG good candidates for future studies aiming at revealing structural modifications to meniscus due to pathologies.
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17
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Lee JH, Rico-Jimenez JJ, Zhang C, Alex A, Chaney EJ, Barkalifa R, Spillman DR, Marjanovic M, Arp Z, Hood SR, Boppart SA. Simultaneous label-free autofluorescence and multi-harmonic imaging reveals in vivo structural and metabolic changes in murine skin. BIOMEDICAL OPTICS EXPRESS 2019; 10:5431-5444. [PMID: 31646056 PMCID: PMC6788598 DOI: 10.1364/boe.10.005431] [Citation(s) in RCA: 6] [Impact Index Per Article: 1.2] [Reference Citation Analysis] [Abstract] [Track Full Text] [Subscribe] [Scholar Register] [Received: 08/01/2019] [Revised: 09/11/2019] [Accepted: 09/24/2019] [Indexed: 05/10/2023]
Abstract
Simultaneous quantification of multifarious cellular metabolites and the extracellular matrix in vivo has been long sought. Simultaneous label-free autofluorescence and multi-harmonic (SLAM) microscopy has achieved simultaneous four-channel nonlinear imaging to study tissue structure and metabolism. In this study, we implemented two laser systems and directly compared SLAM microscopy with conventional two-photon microscopy for in vivo imaging. We found that three-photon imaging of adenine dinucleotide (phosphate) (NAD(P)H) in SLAM microscopy using our tailored laser source provided better resolution, contrast, and background suppression than conventional two-photon imaging of NAD(P)H. We also integrated fluorescence lifetime imaging with SLAM microscopy, and enabled differentiation of free and bound NAD(P)H. We imaged murine skin in vivo and showed that changes in tissue structure, cell dynamics, and metabolism can be monitored simultaneously in real-time. We also discovered an increase in metabolism and protein-bound NAD(P)H in skin cells during the early stages of wound healing.
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Affiliation(s)
- Jang Hyuk Lee
- Center for Optical Molecular Imaging, Beckman Institute for Advanced Science and Technology, University of Illinois at Urbana-Champaign, Urbana, IL 61801, USA
- Co-first authors with equal contribution
| | - Jose J. Rico-Jimenez
- Center for Optical Molecular Imaging, Beckman Institute for Advanced Science and Technology, University of Illinois at Urbana-Champaign, Urbana, IL 61801, USA
- Co-first authors with equal contribution
| | - Chi Zhang
- Center for Optical Molecular Imaging, Beckman Institute for Advanced Science and Technology, University of Illinois at Urbana-Champaign, Urbana, IL 61801, USA
| | - Aneesh Alex
- GlaxoSmithKline, Collegeville, PA 19426, USA
| | - Eric J. Chaney
- Center for Optical Molecular Imaging, Beckman Institute for Advanced Science and Technology, University of Illinois at Urbana-Champaign, Urbana, IL 61801, USA
| | - Ronit Barkalifa
- Center for Optical Molecular Imaging, Beckman Institute for Advanced Science and Technology, University of Illinois at Urbana-Champaign, Urbana, IL 61801, USA
| | - Darold R. Spillman
- Center for Optical Molecular Imaging, Beckman Institute for Advanced Science and Technology, University of Illinois at Urbana-Champaign, Urbana, IL 61801, USA
| | - Marina Marjanovic
- Center for Optical Molecular Imaging, Beckman Institute for Advanced Science and Technology, University of Illinois at Urbana-Champaign, Urbana, IL 61801, USA
| | - Zane Arp
- GlaxoSmithKline, Collegeville, PA 19426, USA
| | | | - Stephen A. Boppart
- Center for Optical Molecular Imaging, Beckman Institute for Advanced Science and Technology, University of Illinois at Urbana-Champaign, Urbana, IL 61801, USA
- Department of Electrical and Computer Engineering, University of Illinois at Urbana-Champaign, Urbana, IL 61801, USA
- Department of Bioengineering, University of Illinois at Urbana-Champaign, Urbana, IL 61801, USA
- Carle Illinois College of Medicine, University of Illinois at Urbana-Champaign, Urbana, IL 61820, USA
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18
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BOYANICH R, BECKER T, CHEN F, KIRK TB, ALLISON G, WU J. Application of confocal, SHG and atomic force microscopy for characterizing the structure of the most superficial layer of articular cartilage. J Microsc 2019; 275:159-171. [DOI: 10.1111/jmi.12824] [Citation(s) in RCA: 4] [Impact Index Per Article: 0.8] [Reference Citation Analysis] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Received: 01/31/2019] [Revised: 06/29/2019] [Accepted: 07/03/2019] [Indexed: 01/19/2023]
Affiliation(s)
- R. BOYANICH
- School of Civil and Mechanical EngineeringCurtin University Perth Western Australia Australia
| | - T. BECKER
- School of Molecular and Life Sciences/Curtin Institute for Functional Molecules and InterfacesCurtin University Perth Western Australia Australia
| | - F. CHEN
- Department of Biomedical EngineeringSouthern University of Science and Technology (SUSTech) Shenzhen China
| | - T. B. KIRK
- School of Civil and Mechanical EngineeringCurtin University Perth Western Australia Australia
| | - G. ALLISON
- Research Office at CurtinCurtin University Perth Western Australia Australia
| | - J.‐P. WU
- Academy of Advanced Interdisciplinary StudiesSouthern University of Science and Technology (SUSTech) Shenzhen China
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19
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Jenkins TL, Little D. Synthetic scaffolds for musculoskeletal tissue engineering: cellular responses to fiber parameters. NPJ Regen Med 2019; 4:15. [PMID: 31263573 PMCID: PMC6597555 DOI: 10.1038/s41536-019-0076-5] [Citation(s) in RCA: 98] [Impact Index Per Article: 19.6] [Reference Citation Analysis] [Abstract] [Key Words] [Grants] [Track Full Text] [Download PDF] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Received: 11/04/2018] [Accepted: 05/14/2019] [Indexed: 12/14/2022] Open
Abstract
Tissue engineering often uses synthetic scaffolds to direct cell responses during engineered tissue development. Since cells reside within specific niches of the extracellular matrix, it is important to understand how the matrix guides cell response and then incorporate this knowledge into scaffold design. The goal of this review is to review elements of cell-matrix interactions that are critical to informing and evaluating cellular response on synthetic scaffolds. Therefore, this review examines fibrous proteins of the extracellular matrix and their effects on cell behavior, followed by a discussion of the cellular responses elicited by fiber diameter, alignment, and scaffold porosity of two dimensional (2D) and three dimensional (3D) synthetic scaffolds. Variations in fiber diameter, alignment, and scaffold porosity guide stem cells toward different lineages. Cells generally exhibit rounded morphology on nanofibers, randomly oriented fibers, and low-porosity scaffolds. Conversely, cells exhibit elongated, spindle-shaped morphology on microfibers, aligned fibers, and high-porosity scaffolds. Cells migrate with higher velocities on nanofibers, aligned fibers, and high-porosity scaffolds but migrate greater distances on microfibers, aligned fibers, and highly porous scaffolds. Incorporating relevant biomimetic factors into synthetic scaffolds destined for specific tissue application could take advantage of and further enhance these responses.
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Affiliation(s)
- Thomas Lee Jenkins
- Department of Biomedical Engineering, Purdue University, West Lafayette, IN 47907 USA
| | - Dianne Little
- Department of Biomedical Engineering, Purdue University, West Lafayette, IN 47907 USA
- Department of Basic Medical Sciences, Purdue University, West Lafayette, IN 47907 USA
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20
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Reed DA, Yotsuya M, Gubareva P, Toth PT, Bertagna A. Two-photon fluorescence and second harmonic generation characterization of extracellular matrix remodeling in post-injury murine temporomandibular joint osteoarthritis. PLoS One 2019; 14:e0214072. [PMID: 30897138 PMCID: PMC6428409 DOI: 10.1371/journal.pone.0214072] [Citation(s) in RCA: 13] [Impact Index Per Article: 2.6] [Reference Citation Analysis] [Abstract] [MESH Headings] [Grants] [Track Full Text] [Download PDF] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Received: 08/22/2018] [Accepted: 03/06/2019] [Indexed: 12/28/2022] Open
Abstract
End stage temporomandibular joint osteoarthritis (TMJ-OA) is characterized by fibrillations, fissures, clefts, and erosion of the mandibular condylar cartilage. The goal of this study was to define changes in pericellular and interterritorial delineations of the extracellular matrix (ECM) that occur preceding and concurrent with the development of this end stage degeneration in a murine surgical instability model. Two-photon fluorescence (TPF) and second harmonic generation (SHG) microscopy was used to evaluate TMJ-OA mediated changes in the ECM. We illustrate that TPF/SHG microscopy reconstructs the three-dimensional network of key fibrillar and micro-fibrillar collagens altered during the progression of TMJ-OA. This method not only generates spatially distinct pericellular and interterritorial delineations of the ECM but distinguishes early and end stage TMJ-OA by signal organization, orientation, and composition. Early stage TMJ-OA at 4- and 8-weeks post-injury is characterized by two structurally distinct regions containing dense, large fiber collagens and superficial, small fiber collagens rich in types I, III, and VI collagen oriented along the mesiodistal axis of the condyle. At 8-weeks post-injury, type VI collagen is locally diminished on the central and medial condyle, but the type I/III rich superficial layer is still present. Twelve- and 16-weeks post-injury mandibular cartilage is characteristic of end-stage disease, with hypocellularity and fibrillations, fissures, and clefts in the articular layer that propagate along the mediolateral axis of the MCC. We hypothesize that the localized depletion of interterritorial and pericellular type VI collagen may signify an early marker for the transition from early to end stage TMJ-OA, influence the injury response of the tissue, and underlie patterns of degeneration that follow attritional modes of failure.
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Affiliation(s)
- David A. Reed
- University of Illinois at Chicago, Department of Oral Biology, Chicago, United States of America
| | - Mamoru Yotsuya
- University of Illinois at Chicago, Department of Oral Biology, Chicago, United States of America
- Tokyo Dental College, Department of Fixed Prosthodontics, Tokyo, Japan
| | - Polina Gubareva
- University of Illinois at Chicago, Department of Oral Biology, Chicago, United States of America
| | - Peter T. Toth
- University of Illinois at Chicago, Research Resources Center Imaging Core, Chicago, United States of America
| | - Andrew Bertagna
- University of Illinois at Chicago, Department of Oral Biology, Chicago, United States of America
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21
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Feneck EM, Lewis PN, Ralphs J, Meek KM. A comparative study of the elastic fibre system within the mouse and human cornea. Exp Eye Res 2018; 177:35-44. [PMID: 30053442 PMCID: PMC6280038 DOI: 10.1016/j.exer.2018.07.024] [Citation(s) in RCA: 17] [Impact Index Per Article: 2.8] [Reference Citation Analysis] [Abstract] [Key Words] [Track Full Text] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Received: 03/16/2018] [Revised: 06/11/2018] [Accepted: 07/21/2018] [Indexed: 01/26/2023]
Abstract
The cornea relies on its organised extracellular matrix for maintaining transparency and biomechanical strength. Studies have identified an elastic fibre system within the human posterior cornea, thought to allow for slight deformations in response to internal pressure fluctuations within the eye. However, the type of elastic fibres that exist within the cornea and their roles remain elusive. The aim of this study was to compare the distribution and organisation of the elastic fibres within the posterior peripheral mouse and human cornea, and elucidate how these fibres integrate with the trabecular meshwork, whilst characterising the distribution of their main likely components (fibrillin-1, elastin and type VI collagen) in different parts of the cornea and adjacent sclera. We identified key differences in the elastic fibre system between the human and mouse cornea. True elastic fibres (containing elastin) were identified within the human posterior peripheral cornea. Elastic fibres appeared to present as an extensive network throughout the mouse corneal stroma, but as fibrillin-rich microfibril bundles rather than true elastic fibres. However, tropoelastin staining indicated the possibility that true elastic fibres had yet to develop in the young mice studied. Differences were also apparent within the anatomy of the trabecular meshwork. The human trabecular meshwork appeared to insert between the corneal stroma and Descemet's membrane, with elastic fibres continuing into the stroma from the trabecular meshwork anterior to Descemet's membrane. Within the mouse cornea, no clear insertion point of the trabecular meshwork was seen, instead the elastic fibres within the trabecular meshwork continued into Descemet's membrane, with the trabecular meshwork joining posterior to Descemet's membrane. True Elastic fibres (containing elastin) occur within the human posterior peripheral cornea. A fibrillin-rich microfibril system was found throughout the mouse corneal stroma, with no apparent true elastic fibres. Human trabecular meshwork inserts between the posterior corneal stroma and Descemet's membrane. A continuity of elastic fibres was identified between cornea and trabecular meshwork in both species.
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Affiliation(s)
- Eleanor M Feneck
- Structural Biophysics Research Group, School of Optometry and Vision Sciences, Cardiff University, Maindy Road, Cardiff, CF24 4HQ, UK
| | - Philip N Lewis
- Structural Biophysics Research Group, School of Optometry and Vision Sciences, Cardiff University, Maindy Road, Cardiff, CF24 4HQ, UK
| | - Jim Ralphs
- School of Biosciences, Cardiff University, Cathays Park, Cardiff, CF10 3AX, UK
| | - Keith M Meek
- Structural Biophysics Research Group, School of Optometry and Vision Sciences, Cardiff University, Maindy Road, Cardiff, CF24 4HQ, UK.
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22
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CHIVERTON J, KAO A, ROLDO M, TOZZI G. Automatic diameter and orientation distribution determination of fibrous materials in micro X-ray CT imaging data. J Microsc 2018; 272:180-195. [DOI: 10.1111/jmi.12719] [Citation(s) in RCA: 7] [Impact Index Per Article: 1.2] [Reference Citation Analysis] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Received: 02/04/2018] [Accepted: 05/10/2018] [Indexed: 11/29/2022]
Affiliation(s)
- J.P. CHIVERTON
- School of Engineering; University of Portsmouth; Portsmouth UK
| | - A. KAO
- School of Engineering; University of Portsmouth; Portsmouth UK
| | - M. ROLDO
- School of Pharmacy and Institute of Biomedical and Biomolecular Science; University of Portsmouth; Portsmouth UK
| | - G. TOZZI
- School of Engineering; University of Portsmouth; Portsmouth UK
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23
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Kiss N, Haluszka D, Lőrincz K, Kuroli E, Hársing J, Mayer B, Kárpáti S, Fekete G, Szipőcs R, Wikonkál N, Medvecz M. Ex vivo nonlinear microscopy imaging of Ehlers-Danlos syndrome-affected skin. Arch Dermatol Res 2018; 310:463-473. [PMID: 29725758 DOI: 10.1007/s00403-018-1835-7] [Citation(s) in RCA: 4] [Impact Index Per Article: 0.7] [Reference Citation Analysis] [Abstract] [Key Words] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Received: 11/15/2017] [Revised: 04/19/2018] [Accepted: 04/25/2018] [Indexed: 10/17/2022]
Abstract
Ehlers-Danlos syndrome (EDS) is the name for a heterogenous group of rare genetic connective tissue disorders with an overall incidence of 1 in 5000. The histological characteristics of EDS have been previously described in detail in the late 1970s and early 1980s. Since that time, the classification of EDS has undergone significant changes, yet the description of the histological features of collagen morphology in different EDS subtypes has endured the test of time. Nonlinear microscopy techniques can be utilized for non-invasive in vivo label-free imaging of the skin. Among these techniques, two-photon absorption fluorescence (TPF) microscopy can visualize endogenous fluorophores, such as elastin, while the morphology of collagen fibers can be assessed by second-harmonic generation (SHG) microscopy. In our present work, we performed TPF and SHG microscopy imaging on ex vivo skin samples of one patient with classical EDS and two patients with vascular EDS and two healthy controls. We detected irregular, loosely dispersed collagen fibers in a non-parallel arrangement in the dermis of the EDS patients, while as expected, there was no noticeable impairment in the elastin content. Based on further studies on a larger number of patients, in vivo nonlinear microscopic imaging could be utilized for the assessment of the skin status of EDS patients in the future.
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Affiliation(s)
- Norbert Kiss
- Department of Dermatology, Venereology and Dermatooncology, Semmelweis University, 41 Mária Street, Budapest, 1085, Hungary.,Institute for Solid State Physics and Optics, Wigner RCP, Budapest, Hungary
| | - Dóra Haluszka
- Department of Dermatology, Venereology and Dermatooncology, Semmelweis University, 41 Mária Street, Budapest, 1085, Hungary.,Institute for Solid State Physics and Optics, Wigner RCP, Budapest, Hungary
| | - Kende Lőrincz
- Department of Dermatology, Venereology and Dermatooncology, Semmelweis University, 41 Mária Street, Budapest, 1085, Hungary
| | - Enikő Kuroli
- Department of Dermatology, Venereology and Dermatooncology, Semmelweis University, 41 Mária Street, Budapest, 1085, Hungary
| | - Judit Hársing
- Department of Dermatology, Venereology and Dermatooncology, Semmelweis University, 41 Mária Street, Budapest, 1085, Hungary
| | - Balázs Mayer
- Department of Dermatology, Venereology and Dermatooncology, Semmelweis University, 41 Mária Street, Budapest, 1085, Hungary
| | - Sarolta Kárpáti
- Department of Dermatology, Venereology and Dermatooncology, Semmelweis University, 41 Mária Street, Budapest, 1085, Hungary
| | - György Fekete
- 2nd Department of Pediatrics, Semmelweis University, Budapest, Hungary
| | - Róbert Szipőcs
- Institute for Solid State Physics and Optics, Wigner RCP, Budapest, Hungary.,R&D Ultrafast Lasers Ltd, P.O. Box 622, Budapest, 1539, Hungary
| | - Norbert Wikonkál
- Department of Dermatology, Venereology and Dermatooncology, Semmelweis University, 41 Mária Street, Budapest, 1085, Hungary
| | - Márta Medvecz
- Department of Dermatology, Venereology and Dermatooncology, Semmelweis University, 41 Mária Street, Budapest, 1085, Hungary.
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24
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Chronic cigarette smoke exposure drives spiral ganglion neuron loss in mice. Sci Rep 2018; 8:5746. [PMID: 29636532 PMCID: PMC5893541 DOI: 10.1038/s41598-018-24166-9] [Citation(s) in RCA: 6] [Impact Index Per Article: 1.0] [Reference Citation Analysis] [Abstract] [Track Full Text] [Download PDF] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Received: 12/18/2017] [Accepted: 03/28/2018] [Indexed: 02/07/2023] Open
Abstract
Tobacco use is associated with an increased risk of hearing loss in older individuals, suggesting cigarette smoke (CS) exposure may target the peripheral auditory organs. However, the effects of CS exposure on general cochlear anatomy have not previously been explored. Here we compare control and chronic CS exposed cochleae from adult mice to assess changes in structure and cell survival. Two-photon imaging techniques, including the imaging of second harmonic generation (SHG) and two-photon excitation fluorescence (TPEF) from native molecules, were used to probe the whole cochlear organ for changes. We found evidence for fibrillar collagen accumulation in the spiral ganglion and organ of Corti, consistent with fibrosis. Quantitative TPEF indicated that basal CS-exposed spiral ganglion neurons experienced greater oxidative stress than control neurons, which was confirmed by histological staining for lipid peroxidation products. Cell counts confirmed that the CS-exposed spiral ganglion also contained fewer basal neurons. Taken together, these data support the premise that CS exposure induces oxidative stress in cochlear cells. They also indicate that two-photon techniques may screen cochlear tissues for oxidative stress.
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25
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Albro MB, Bergholt MS, St-Pierre JP, Vinals Guitart A, Zlotnick HM, Evita EG, Stevens MM. Raman spectroscopic imaging for quantification of depth-dependent and local heterogeneities in native and engineered cartilage. NPJ Regen Med 2018; 3:3. [PMID: 29449966 PMCID: PMC5807411 DOI: 10.1038/s41536-018-0042-7] [Citation(s) in RCA: 46] [Impact Index Per Article: 7.7] [Reference Citation Analysis] [Abstract] [Grants] [Track Full Text] [Download PDF] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Received: 06/28/2017] [Revised: 01/08/2018] [Accepted: 01/10/2018] [Indexed: 12/11/2022] Open
Abstract
Articular cartilage possesses a remarkable, mechanically-robust extracellular matrix (ECM) that is organized and distributed throughout the tissue to resist physiologic strains and provide low friction during articulation. The ability to characterize the make-up and distribution of the cartilage ECM is critical to both understand the process by which articular cartilage undergoes disease-related degeneration and to develop novel tissue repair strategies to restore tissue functionality. However, the ability to quantitatively measure the spatial distribution of cartilage ECM constituents throughout the tissue has remained a major challenge. In this experimental investigation, we assessed the analytical ability of Raman micro-spectroscopic imaging to semi-quantitatively measure the distribution of the major ECM constituents in cartilage tissues. Raman spectroscopic images were acquired of two distinct cartilage tissue types that possess large spatial ECM gradients throughout their depth: native articular cartilage explants and large engineered cartilage tissue constructs. Spectral acquisitions were processed via multivariate curve resolution to decompose the "fingerprint" range spectra (800-1800 cm-1) to the component spectra of GAG, collagen, and water, giving rise to the depth dependent concentration profile of each constituent throughout the tissues. These Raman spectroscopic acquired-profiles exhibited strong agreement with profiles independently acquired via direct biochemical assaying of spatial tissue sections. Further, we harness this spectroscopic technique to evaluate local heterogeneities through the depth of cartilage. This work represents a powerful analytical validation of the accuracy of Raman spectroscopic imaging measurements of the spatial distribution of biochemical components in a biological tissue and shows that it can be used as a valuable tool for quantitatively measuring the distribution and organization of ECM constituents in native and engineered cartilage tissue specimens.
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Affiliation(s)
- M. B. Albro
- Department of Materials, Imperial College London, London, SW7 2AZ United Kingdom
- Department of Bioengineering, Imperial College London, London, SW7 2AZ United Kingdom
- Institute of Biomedical Engineering, Imperial College London, London, SW7 2AZ United Kingdom
| | - M. S. Bergholt
- Department of Materials, Imperial College London, London, SW7 2AZ United Kingdom
- Department of Bioengineering, Imperial College London, London, SW7 2AZ United Kingdom
- Institute of Biomedical Engineering, Imperial College London, London, SW7 2AZ United Kingdom
| | - J. P. St-Pierre
- Department of Materials, Imperial College London, London, SW7 2AZ United Kingdom
- Department of Bioengineering, Imperial College London, London, SW7 2AZ United Kingdom
- Institute of Biomedical Engineering, Imperial College London, London, SW7 2AZ United Kingdom
| | - A. Vinals Guitart
- Department of Materials, Imperial College London, London, SW7 2AZ United Kingdom
- Department of Bioengineering, Imperial College London, London, SW7 2AZ United Kingdom
- Institute of Biomedical Engineering, Imperial College London, London, SW7 2AZ United Kingdom
| | - H. M. Zlotnick
- Department of Materials, Imperial College London, London, SW7 2AZ United Kingdom
- Department of Bioengineering, Imperial College London, London, SW7 2AZ United Kingdom
- Institute of Biomedical Engineering, Imperial College London, London, SW7 2AZ United Kingdom
| | - E. G. Evita
- Department of Materials, Imperial College London, London, SW7 2AZ United Kingdom
- Department of Bioengineering, Imperial College London, London, SW7 2AZ United Kingdom
- Institute of Biomedical Engineering, Imperial College London, London, SW7 2AZ United Kingdom
| | - M. M. Stevens
- Department of Materials, Imperial College London, London, SW7 2AZ United Kingdom
- Department of Bioengineering, Imperial College London, London, SW7 2AZ United Kingdom
- Institute of Biomedical Engineering, Imperial College London, London, SW7 2AZ United Kingdom
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26
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Zyablitskaya M, Munteanu EL, Nagasaki T, Paik DC. Second Harmonic Generation Signals in Rabbit Sclera As a Tool for Evaluation of Therapeutic Tissue Cross-linking (TXL) for Myopia. J Vis Exp 2018. [PMID: 29364259 DOI: 10.3791/56385] [Citation(s) in RCA: 3] [Impact Index Per Article: 0.5] [Reference Citation Analysis] [Abstract] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Indexed: 12/28/2022] Open
Abstract
Methods to strengthen tissue by introducing chemical bonds (non-enzymatic cross-linking) into structural proteins (fibrillar collagens) for therapy include photochemical cross-linking and tissue cross-linking (TXL) methods. Such methods for inducing mechanical tissue property changes are being employed to the cornea in corneal thinning (mechanically weakened) disorders such as keratoconus as well as the sclera in progressive myopia, where thinning and weakening of the posterior sclera occurs and likely contributes to axial elongation. The primary target proteins for such tissue strengthening are fibrillar collagens which constitute the great majority of dry weight proteins in the cornea and sclera. Fortuitously, fibrillar collagens are the main source of second harmonic generation signals in the tissue extracellular space. Therefore, modifications of the collagen proteins, such as those induced through cross-linking therapies, could potentially be detected and quantitated through the use of second harmonic generation microscopy (SHGM). Monitoring SHGM signals through the use of a laser scanning microscopy system coupled with an infrared excitation light source is an exciting modern imaging method that is enjoying widespread usage in the biomedical sciences. Thus, the present study was undertaken in order to evaluate the use of SHGM microscopy as a means to measure induced cross-linking effects in ex vivo rabbit sclera, following an injection of a chemical cross-linking agent into the sub-Tenon's space (sT), an injection approach that is standard practice for causing ocular anesthesia during ophthalmologic clinical procedures. The chemical cross-linking agent, sodium hydroxymethylglycinate (SMG), is from a class of cosmetic preservatives known as formaldehyde releasing agents (FARs). Scleral changes following reaction with SMG resulted in increases in SHG signals and correlated with shifts in thermal denaturation temperature, a standard method for evaluating induced tissue cross-linking effects.
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Affiliation(s)
- Mariya Zyablitskaya
- Department of Ophthalmology, Columbia University College of Physicians and Surgeons
| | - E Laura Munteanu
- Confocal and Specialized Microscopy Shared Resource, Herbert Irving Comprehensive Cancer Center, Columbia University
| | - Takayuki Nagasaki
- Department of Ophthalmology, Columbia University College of Physicians and Surgeons
| | - David C Paik
- Department of Ophthalmology, Columbia University College of Physicians and Surgeons;
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27
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Querido W, Falcon JM, Kandel S, Pleshko N. Vibrational spectroscopy and imaging: applications for tissue engineering. Analyst 2017; 142:4005-4017. [PMID: 28956032 PMCID: PMC5653442 DOI: 10.1039/c7an01055a] [Citation(s) in RCA: 18] [Impact Index Per Article: 2.6] [Reference Citation Analysis] [Abstract] [MESH Headings] [Grants] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Indexed: 12/11/2022]
Abstract
Tissue engineering (TE) approaches strive to regenerate or replace an organ or tissue. The successful development and subsequent integration of a TE construct is contingent on a series of in vitro and in vivo events that result in an optimal construct for implantation. Current widely used methods for evaluation of constructs are incapable of providing an accurate compositional assessment without destruction of the construct. In this review, we discuss the contributions of vibrational spectroscopic assessment for evaluation of tissue engineered construct composition, both during development and post-implantation. Fourier transform infrared (FTIR) spectroscopy in the mid and near-infrared range, as well as Raman spectroscopy, are intrinsically label free, can be non-destructive, and provide specific information on the chemical composition of tissues. Overall, we examine the contribution that vibrational spectroscopy via fiber optics and imaging have to tissue engineering approaches.
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Affiliation(s)
- William Querido
- Department of Bioengineering, Temple University, Philadelphia, PA, USA.
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28
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Kim M, Farrell MJ, Steinberg DR, Burdick JA, Mauck RL. Enhanced nutrient transport improves the depth-dependent properties of tri-layered engineered cartilage constructs with zonal co-culture of chondrocytes and MSCs. Acta Biomater 2017. [PMID: 28629894 DOI: 10.1016/j.actbio.2017.06.025] [Citation(s) in RCA: 21] [Impact Index Per Article: 3.0] [Reference Citation Analysis] [Abstract] [Key Words] [MESH Headings] [Grants] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Indexed: 01/22/2023]
Abstract
Biomimetic design in cartilage tissue engineering is a challenge given the complexity of the native tissue. While numerous studies have generated constructs with near-native bulk properties, recapitulating the depth-dependent features of native tissue remains a challenge. Furthermore, limitations in nutrient transport and matrix accumulation in engineered constructs hinders maturation within the central core of large constructs. To overcome these limitations, we fabricated tri-layered constructs that recapitulate the depth-dependent cellular organization and functional properties of native tissue using zonally derived chondrocytes co-cultured with MSCs. We also introduced porous hollow fibers (HFs) and HFs/cotton threads to enhance nutrient transport. Our results showed that tri-layered constructs with depth-dependent organization and properties could be fabricated. The addition of HFs or HFs/threads improved matrix accumulation in the central core region. With HF/threads, the local modulus in the deep region of tri-layered constructs nearly matched that of native tissue, though the properties in the central regions remained lower. These constructs reproduced the zonal organization and depth-dependent properties of native tissue, and demonstrate that a layer-by-layer fabrication scheme holds promise for the biomimetic repair of focal cartilage defects. STATEMENT OF SIGNIFICANCE Articular cartilage is a highly organized tissue driven by zonal heterogeneity of cells, extracellular matrix proteins and fibril orientations, resulting in depth-dependent mechanical properties. Therefore, the recapitulation of the functional properties of native cartilage in a tissue engineered construct requires such a biomimetic design of the morphological organization, and this has remained a challenge in cartilage tissue engineering. This study demonstrates that a layer-by-layer fabrication scheme, including co-cultures of zone-specific articular CHs and MSCs, can reproduce the depth-dependent characteristics and mechanical properties of native cartilage while minimizing the need for large numbers of chondrocytes. In addition, introduction of a porous hollow fiber (combined with a cotton thread) enhanced nutrient transport and depth-dependent properties of the tri-layered construct. Such a tri-layered construct may provide critical advantages for focal cartilage repair. These constructs hold promise for restoring native tissue structure and function, and may be beneficial in terms of zone-to-zone integration with adjacent host tissue and providing more appropriate strain transfer after implantation.
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Affiliation(s)
- Minwook Kim
- McKay Orthopaedic Research Laboratory, Department of Orthopaedic Surgery, Perelman School of Medicine, University of Pennsylvania, Philadelphia, PA 19104, USA; Department of Bioengineering, University of Pennsylvania, Philadelphia, PA 19104, USA; Translational Musculoskeletal Research Center (TMRC), Corporal Michael J. Crescenz Veterans Affairs Medical Center, Philadelphia, PA 19104, USA
| | - Megan J Farrell
- McKay Orthopaedic Research Laboratory, Department of Orthopaedic Surgery, Perelman School of Medicine, University of Pennsylvania, Philadelphia, PA 19104, USA; Department of Bioengineering, University of Pennsylvania, Philadelphia, PA 19104, USA; Translational Musculoskeletal Research Center (TMRC), Corporal Michael J. Crescenz Veterans Affairs Medical Center, Philadelphia, PA 19104, USA
| | - David R Steinberg
- McKay Orthopaedic Research Laboratory, Department of Orthopaedic Surgery, Perelman School of Medicine, University of Pennsylvania, Philadelphia, PA 19104, USA; Translational Musculoskeletal Research Center (TMRC), Corporal Michael J. Crescenz Veterans Affairs Medical Center, Philadelphia, PA 19104, USA
| | - Jason A Burdick
- Department of Bioengineering, University of Pennsylvania, Philadelphia, PA 19104, USA; Translational Musculoskeletal Research Center (TMRC), Corporal Michael J. Crescenz Veterans Affairs Medical Center, Philadelphia, PA 19104, USA
| | - Robert L Mauck
- McKay Orthopaedic Research Laboratory, Department of Orthopaedic Surgery, Perelman School of Medicine, University of Pennsylvania, Philadelphia, PA 19104, USA; Department of Bioengineering, University of Pennsylvania, Philadelphia, PA 19104, USA; Translational Musculoskeletal Research Center (TMRC), Corporal Michael J. Crescenz Veterans Affairs Medical Center, Philadelphia, PA 19104, USA.
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29
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Zyablitskaya M, Takaoka A, Munteanu EL, Nagasaki T, Trokel SL, Paik DC. Evaluation of Therapeutic Tissue Crosslinking (TXL) for Myopia Using Second Harmonic Generation Signal Microscopy in Rabbit Sclera. Invest Ophthalmol Vis Sci 2017; 58:21-29. [PMID: 28055099 PMCID: PMC5225996 DOI: 10.1167/iovs.16-20241] [Citation(s) in RCA: 23] [Impact Index Per Article: 3.3] [Reference Citation Analysis] [Abstract] [Track Full Text] [Download PDF] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Indexed: 01/15/2023] Open
Abstract
Purpose Second harmonic generation signals (SHG) are emitted preferentially from collagenous tissue structures and have been used to evaluate photochemically-induced (CXL) crosslinking changes in the cornea. Since therapeutic tissue crosslinking (TXL) using sodium hydroxymethylglycinate (SMG) of the sclera is a potential treatment for high myopia, we explored the use of SHG microscopy to evaluate the effects. Methods Single sub-Tenon's (sT) injections (400 μL) using SMG (40-400 mM) were made at the equatorial 12 o'clock position of the right eye of cadaveric rabbit heads (n = 16 pairs). After 3.5 hours, confocal microscopy (CM) was performed using 860 nm two-photon excitation and 400 to 450 nm emission. Pixel density and fiber bundle "waviness" analyses were performed on the images. Crosslinking effects were confirmed using thermal denaturation (Tm) temperature. Comparison experiments with riboflavin photochemical crosslinking were done. Results Therapeutic tissue crosslinking localization studies indicated that crosslinking changes occurred at the site of injection and in adjacent sectors. Second harmonic generation signals revealed large fibrous collagenous bundled structures that displayed various degrees of waviness. Histogram analysis showed a nearly 6-fold signal increase in 400 mM SMG over 40 mM. This corresponded to a ΔTm = 13°C for 400 mM versus ΔTm = 4°C for 40 mM. Waviness analysis indicated increased fiber straightening as a result of SMG CXL. Conclusions Second harmonic generation signal intensity and fiber bundle waviness is altered by scleral tissue crosslinking using SMG. These changes provide insights into the macromolecular changes that are induced by therapeutic crosslinking technology and may provide a method to evaluate connective tissue protein changes induced by scleral crosslinking therapies.
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Affiliation(s)
- Mariya Zyablitskaya
- Department of Ophthalmology, Columbia University College of Physicians and Surgeons, New York, New York, United States
| | - Anna Takaoka
- Department of Ophthalmology, Columbia University College of Physicians and Surgeons, New York, New York, United States
| | - Emilia L Munteanu
- Confocal and Specialized Microscopy Shared Resource, Herbert Irving Comprehensive Cancer Center, Columbia University, New York, New York, United States
| | - Takayuki Nagasaki
- Department of Ophthalmology, Columbia University College of Physicians and Surgeons, New York, New York, United States
| | - Stephen L Trokel
- Department of Ophthalmology, Columbia University College of Physicians and Surgeons, New York, New York, United States
| | - David C Paik
- Department of Ophthalmology, Columbia University College of Physicians and Surgeons, New York, New York, United States
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30
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Pang X, Wu JP, Allison GT, Xu J, Rubenson J, Zheng MH, Lloyd DG, Gardiner B, Wang A, Kirk TB. Three dimensional microstructural network of elastin, collagen, and cells in Achilles tendons. J Orthop Res 2017; 35:1203-1214. [PMID: 27002477 DOI: 10.1002/jor.23240] [Citation(s) in RCA: 35] [Impact Index Per Article: 5.0] [Reference Citation Analysis] [Abstract] [Key Words] [Track Full Text] [Journal Information] [Submit a Manuscript] [Subscribe] [Scholar Register] [Received: 06/26/2015] [Accepted: 03/17/2016] [Indexed: 02/04/2023]
Abstract
Similar to most biological tissues, the biomechanical, and functional characteristics of the Achilles tendon are closely related to its composition and microstructure. It is commonly reported that type I collagen is the predominant component of tendons and is mainly responsible for the tissue's function. Although elastin has been found in varying proportions in other connective tissues, previous studies report that tendons contain very small quantities of elastin. However, the morphology and the microstructural relationship among the elastic fibres, collagen, and cells in tendon tissue have not been well examined. We hypothesize the elastic fibres, as another fibrillar component in the extracellular matrix, have a unique role in mechanical function and microstructural arrangement in Achilles tendons. It has been shown that elastic fibres present a close connection with the tenocytes. The close relationship of the three components has been revealed as a distinct, integrated and complex microstructural network. Notably, a "spiral" structure within fibril bundles in Achilles tendons was observed in some samples in specialized regions. This study substantiates the hierarchical system of the spatial microstructure of tendon, including the mapping of collagen, elastin and tenocytes, with 3-dimensional confocal images. © 2017 Orthopaedic Research Society. Published by Wiley Periodicals, Inc. J Orthop Res 35:1203-1214, 2017.
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Affiliation(s)
- Xin Pang
- Department of Mechanical Engineering, 3D Imaging and Bioengineering Laboratory, Curtin University, Bentley, Western Australia 6102, Australia
| | - Jian-Ping Wu
- Department of Mechanical Engineering, 3D Imaging and Bioengineering Laboratory, Curtin University, Bentley, Western Australia 6102, Australia
| | - Garry T Allison
- The School of Physiotherapy and Exercise Sciences, Curtin University, Western Australia, Australia
| | - Jiake Xu
- The School of Pathology and Laboratory Medicine, University of Western Australia, Western Australia, Australia
| | - Jonas Rubenson
- Department of Kinesiology, Pennsylvania State University, Pennsylvania.,School of Sport Science, Exercise and Health, University of Western Australia, Western Australia, Australia
| | - Ming-Hao Zheng
- Centre for Orthopaedic Research, School of Surgery, University of Western Australia, Western Australia, Australia
| | - David G Lloyd
- Centre for Musculoskeletal Research, Menzies Health Institute Queensland, Griffith University, Queensland, Australia
| | - Bruce Gardiner
- School of Engineering and Information Technology, Murdoch University, Western Australia, Australia
| | - Allan Wang
- Centre for Orthopaedic Research, School of Surgery, University of Western Australia, Western Australia, Australia.,St John of God Hospital, Western Australia, Australia
| | - Thomas Brett Kirk
- Department of Mechanical Engineering, 3D Imaging and Bioengineering Laboratory, Curtin University, Bentley, Western Australia 6102, Australia
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31
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Andrews SHJ, Adesida AB, Abusara Z, Shrive NG. Current concepts on structure-function relationships in the menisci. Connect Tissue Res 2017; 58:271-281. [PMID: 28267400 DOI: 10.1080/03008207.2017.1303489] [Citation(s) in RCA: 37] [Impact Index Per Article: 5.3] [Reference Citation Analysis] [Abstract] [Key Words] [Track Full Text] [Journal Information] [Submit a Manuscript] [Subscribe] [Scholar Register] [Indexed: 02/03/2023]
Abstract
The menisci are intricately organized structures that perform many tasks in the knee. We review their structure and function and introduce new data about their tibial and femoral surfaces. As the femur and tibia approach each other when the knee is bearing load, circumferential tension develops in the menisci, enabling the transmission of compressive load between the femoral and tibial cartilage layers. A low shear modulus is necessary for the tissue to adapt its shape to the changing radius of the femur as that bone moves relative to the tibia during joint articulation. The organization of the meniscus facilitates its functions. In the outer region of the menisci, intertwined collagen fibrils, fibers, and fascicles with predominantly circumferential orientation are prevalent; these structures are held together by radial tie fibers and sheets. Toward the inner portion of the menisci, there is more proteoglycan and the structure becomes more cartilage-like. The transition between these structural forms is gradual and seamless. The flexible roots, required for rigid body motion of the menisci, meld with both the tibia and the outer portion of the menisci to maintain continuity for resistance to the circumferential tension. Our new data demonstrate that the femoral and tibial surfaces of the menisci are structurally analogous to the surfaces of articular cartilage, enabling consistent modes of lubrication and load transfer to occur at the interfacing surfaces throughout motion. The structure and function of the menisci are thus shown to be strongly related to one another: form clearly complements function.
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Affiliation(s)
| | | | - Ziad Abusara
- b Faculty of Kinesiology , University of Calgary , Calgary , Canada
| | - Nigel G Shrive
- c McCaig Institute for Bone and Joint Health, and Department of Civil Engineering , University of Calgary , Calgary , Canada
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32
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Bergholt MS, St-Pierre JP, Offeddu GS, Parmar P, Albro MB, Puetzer J, Oyen M, Stevens MM. Raman Spectroscopy Reveals New Insights into the Zonal Organization of Native and Tissue-Engineered Articular Cartilage. ACS CENTRAL SCIENCE 2016; 2:885-895. [PMID: 28058277 PMCID: PMC5200931 DOI: 10.1021/acscentsci.6b00222] [Citation(s) in RCA: 87] [Impact Index Per Article: 10.9] [Reference Citation Analysis] [Abstract] [Grants] [Track Full Text] [Subscribe] [Scholar Register] [Received: 08/10/2016] [Indexed: 05/17/2023]
Abstract
Tissue architecture is intimately linked with its functions, and loss of tissue organization is often associated with pathologies. The intricate depth-dependent extracellular matrix (ECM) arrangement in articular cartilage is critical to its biomechanical functions. In this study, we developed a Raman spectroscopic imaging approach to gain new insight into the depth-dependent arrangement of native and tissue-engineered articular cartilage using bovine tissues and cells. Our results revealed previously unreported tissue complexity into at least six zones above the tidemark based on a principal component analysis and k-means clustering analysis of the distribution and orientation of the main ECM components. Correlation of nanoindentation and Raman spectroscopic data suggested that the biomechanics across the tissue depth are influenced by ECM microstructure rather than composition. Further, Raman spectroscopy together with multivariate analysis revealed changes in the collagen, glycosaminoglycan, and water distributions in tissue-engineered constructs over time. These changes were assessed using simple metrics that promise to instruct efforts toward the regeneration of a broad range of tissues with native zonal complexity and functional performance.
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Affiliation(s)
- Mads S. Bergholt
- Department
of Materials, Imperial College London, London SW7 2AZ, United Kingdom
- Department
of Bioengineering, Imperial College London, London SW7 2AZ, United Kingdom
- Institute
of Biomedical Engineering, Imperial College
London, London SW7 2AZ, United Kingdom
| | - Jean-Philippe St-Pierre
- Department
of Materials, Imperial College London, London SW7 2AZ, United Kingdom
- Department
of Bioengineering, Imperial College London, London SW7 2AZ, United Kingdom
- Institute
of Biomedical Engineering, Imperial College
London, London SW7 2AZ, United Kingdom
| | - Giovanni S. Offeddu
- Nanoscience
Centre, Department of Engineering, University
of Cambridge, Cambridge CB3 0FF, United Kingdom
| | - Paresh
A. Parmar
- Department
of Materials, Imperial College London, London SW7 2AZ, United Kingdom
- Department
of Bioengineering, Imperial College London, London SW7 2AZ, United Kingdom
- Institute
of Biomedical Engineering, Imperial College
London, London SW7 2AZ, United Kingdom
| | - Michael B. Albro
- Department
of Materials, Imperial College London, London SW7 2AZ, United Kingdom
- Department
of Bioengineering, Imperial College London, London SW7 2AZ, United Kingdom
- Institute
of Biomedical Engineering, Imperial College
London, London SW7 2AZ, United Kingdom
| | - Jennifer
L. Puetzer
- Department
of Materials, Imperial College London, London SW7 2AZ, United Kingdom
- Department
of Bioengineering, Imperial College London, London SW7 2AZ, United Kingdom
- Institute
of Biomedical Engineering, Imperial College
London, London SW7 2AZ, United Kingdom
| | - Michelle
L. Oyen
- Nanoscience
Centre, Department of Engineering, University
of Cambridge, Cambridge CB3 0FF, United Kingdom
| | - Molly M. Stevens
- Department
of Materials, Imperial College London, London SW7 2AZ, United Kingdom
- Department
of Bioengineering, Imperial College London, London SW7 2AZ, United Kingdom
- Institute
of Biomedical Engineering, Imperial College
London, London SW7 2AZ, United Kingdom
- E-mail:
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33
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Luo T, Chen H, Kassab GS. 3D reconstruction of elastin fibres in coronary adventitia. J Microsc 2016; 265:121-131. [PMID: 27596327 DOI: 10.1111/jmi.12470] [Citation(s) in RCA: 5] [Impact Index Per Article: 0.6] [Reference Citation Analysis] [Abstract] [Key Words] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Received: 09/10/2015] [Revised: 08/05/2016] [Accepted: 08/07/2016] [Indexed: 02/01/2023]
Abstract
A 3D reconstruction of individual fibres in vascular tissue is necessary to understand the microstructure properties of the vessel wall. The objective of this study is to determine the 3D microstructure of elastin fibres in the adventitia of coronary arteries. Quantification of fibre geometry is challenging due to the complex interwoven structure of the fibres. In particular, accurate linking of gaps remains a significant challenge, and complex features such as long gaps and interwoven fibres have not been adequately addressed by current fibre reconstruction algorithms. We use a novel line Laplacian deformation method, which better deals with fibre shape uncertainty to reconstruct elastin fibres in the coronary adventitia of five swine. A cost function, based on entropy and Euler Spiral, was used in the shortest path search. We find that mean diameter of elastin fibres is 1.67 ± 1.42 μm and fibre orientation is clustered around two major angles of 8.9˚ and 81.8˚. Comparing with CT-FIRE, we find that our method gives more accurate estimation of fibre width. To our knowledge, the measurements obtained using our algorithm represent the first investigation focused on the reconstruction of full elastin fibre length. Our data provide a foundation for a 3D microstructural model of the coronary adventitia to elucidate the structure-function relationship of elastin fibres.
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Affiliation(s)
- T Luo
- Department of Bioengineering, California Medical Innovations Institute, San Diego, California, U.S.A
| | - H Chen
- Department of Bioengineering, California Medical Innovations Institute, San Diego, California, U.S.A
| | - G S Kassab
- Department of Bioengineering, California Medical Innovations Institute, San Diego, California, U.S.A
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34
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Seeger M, Karlas A, Soliman D, Pelisek J, Ntziachristos V. Multimodal optoacoustic and multiphoton microscopy of human carotid atheroma. PHOTOACOUSTICS 2016; 4:102-111. [PMID: 27761409 PMCID: PMC5063356 DOI: 10.1016/j.pacs.2016.07.001] [Citation(s) in RCA: 27] [Impact Index Per Article: 3.4] [Reference Citation Analysis] [Abstract] [Key Words] [Track Full Text] [Subscribe] [Scholar Register] [Received: 03/14/2016] [Revised: 05/14/2016] [Accepted: 07/25/2016] [Indexed: 05/20/2023]
Abstract
Carotid artery atherosclerosis is a main cause of stroke. Understanding atherosclerosis biology is critical in the development of targeted prevention and treatment strategies. Consequently, there is demand for advanced tools investigating atheroma pathology. We consider hybrid optoacoustic and multiphoton microscopy for the integrated and complementary interrogation of plaque tissue constituents and their mutual interactions. Herein, we visualize human carotid plaque using a hybrid multimodal imaging system that combines optical resolution optoacoustic (photoacoustic) microscopy, second and third harmonic generation microscopy, and two-photon excitation fluorescence microscopy. Our data suggest more comprehensive insights in the pathophysiology of atheroma formation and destabilization, by enabling congruent visualization of structural and biological features critical for the atherosclerotic process and its acute complications, such as red blood cells and collagen.
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Key Words
- BF, Brightfield
- CAE, Carotid thrombendarterectomy
- CMR, Continuous multirecord
- Collagen
- DAQ, Data acquisition
- FOV, Field of view
- GM, Galvanometric mirrors
- HE, Hemalaun-Eosin
- Human carotid atheroma
- IPH, Intraplaque hemorrhage
- LDL, Low density lipoprotein
- MAP, Maximum amplitude projection
- MPM, Multiphoton microscopy
- MPOM, Multiphoton and optoacoustic microscopy
- Multimodal microscopy
- NLO, Non-linear optical
- Non-linear optical microscopy
- OAM, Optoacoustic microscopy
- Optoacoustic microscopy
- PMT, Photo multiplier tube
- PSR, Picro-Sirius Red
- Photoacoustic microscopy
- RBC, Red blood cell
- ROI, Region of interest
- Red blood cells
- SHG, Second harmonic generation
- SMC, Smooth muscle cell
- THG, Third harmonic generation
- TPEF, Two-photon excitation fluorescence
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Affiliation(s)
- Markus Seeger
- Chair for Biological Imaging, Technische Universität München, Munich, Germany
- Institute of Biological and Medical Imaging, Helmholtz Zentrum München, Neuherberg, Germany
| | - Angelos Karlas
- Chair for Biological Imaging, Technische Universität München, Munich, Germany
- Institute of Biological and Medical Imaging, Helmholtz Zentrum München, Neuherberg, Germany
- Department of Cardiology, Klinikum rechts der Isar, Technische Universität München, Munich, Germany
| | - Dominik Soliman
- Chair for Biological Imaging, Technische Universität München, Munich, Germany
- Institute of Biological and Medical Imaging, Helmholtz Zentrum München, Neuherberg, Germany
| | - Jaroslav Pelisek
- Department of Vascular and Endovascular Surgery, Klinikum rechts der Isar, Technische Universität München, Munich, Germany
| | - Vasilis Ntziachristos
- Chair for Biological Imaging, Technische Universität München, Munich, Germany
- Institute of Biological and Medical Imaging, Helmholtz Zentrum München, Neuherberg, Germany
- Corresponding author at: Chair for Biological Imaging, Technische Universität München, Munich, Germany and Institute of Biological and Medical Imaging, Helmholtz Zentrum München, Neuherberg, Germany.
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35
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Chen H, Zhao X, Berwick ZC, Krieger JF, Chambers S, Kassab GS. Microstructure and Mechanical Property of Glutaraldehyde-Treated Porcine Pulmonary Ligament. J Biomech Eng 2016; 138:061003. [PMID: 27040732 DOI: 10.1115/1.4033300] [Citation(s) in RCA: 6] [Impact Index Per Article: 0.8] [Reference Citation Analysis] [Abstract] [MESH Headings] [Grants] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Received: 06/22/2015] [Indexed: 01/15/2023]
Abstract
There is a significant need for fixed biological tissues with desired structural and material constituents for tissue engineering applications. Here, we introduce the lung ligament as a fixed biological material that may have clinical utility for tissue engineering. To characterize the lung tissue for potential clinical applications, we studied glutaraldehyde-treated porcine pulmonary ligament (n = 11) with multiphoton microscopy (MPM) and conducted biaxial planar experiments to characterize the mechanical property of the tissue. The MPM imaging revealed that there are generally two families of collagen fibers distributed in two distinct layers: The first family largely aligns along the longitudinal direction with a mean angle of θ = 10.7 ± 9.3 deg, while the second one exhibits a random distribution with a mean θ = 36.6 ± 27.4. Elastin fibers appear in some intermediate sublayers with a random orientation distribution with a mean θ = 39.6 ± 23 deg. Based on the microstructural observation, a microstructure-based constitutive law was proposed to model the elastic property of the tissue. The material parameters were identified by fitting the model to the biaxial stress-strain data of specimens, and good fitting quality was achieved. The parameter e0 (which denotes the strain beyond which the collagen can withstand tension) of glutaraldehyde-treated tissues demonstrated low variability implying a relatively consistent collagen undulation in different samples, while the stiffness parameters for elastin and collagen fibers showed relatively greater variability. The fixed tissues presented a smaller e0 than that of fresh specimen, confirming that glutaraldehyde crosslinking increases the mechanical strength of collagen-based biomaterials. The present study sheds light on the biomechanics of glutaraldehyde-treated porcine pulmonary ligament that may be a candidate for tissue engineering.
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36
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Eisenstein NM, Cox SC, Williams RL, Stapley SA, Grover LM. Bedside, Benchtop, and Bioengineering: Physicochemical Imaging Techniques in Biomineralization. Adv Healthc Mater 2016; 5:507-28. [PMID: 26789418 DOI: 10.1002/adhm.201500617] [Citation(s) in RCA: 5] [Impact Index Per Article: 0.6] [Reference Citation Analysis] [Abstract] [Key Words] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Received: 08/05/2015] [Revised: 09/10/2015] [Indexed: 01/10/2023]
Abstract
The need to quantify physicochemical properties of mineralization spans many fields. Clinicians, mineralization researchers, and bone tissue bioengineers need to be able to measure the distribution, quantity, and the mechanical and chemical properties of mineralization within a wide variety of substrates from injured muscle to electrospun polymer scaffolds and everything in between. The techniques available to measure these properties are highly diverse in terms of their complexity and utility. Therefore it is of the utmost importance that those who intend to use them have a clear understanding of the advantages and disadvantages of each technique and its appropriateness to their specific application. This review provides all of this information for each technique and uses heterotopic ossification and engineered bone substitutes as examples to illustrate how these techniques have been applied. In addition, we provide novel data using advanced techniques to analyze human samples of combat related heterotopic ossification.
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Affiliation(s)
- Neil M. Eisenstein
- Chemical Engineering; University of Birmingham; Edgbaston B15 2TT UK
- Royal Centre for Defence Medicine; ICT Centre; Vincent Drive; Edgbaston B15 2SQ UK
| | - Sophie C. Cox
- Chemical Engineering; University of Birmingham; Edgbaston B15 2TT UK
| | | | - Sarah A. Stapley
- Royal Centre for Defence Medicine; ICT Centre; Vincent Drive; Edgbaston B15 2SQ UK
| | - Liam M. Grover
- Chemical Engineering; University of Birmingham; Edgbaston B15 2TT UK
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Novakofski KD, Pownder SL, Koff MF, Williams RM, Potter HG, Fortier LA. High-Resolution Methods for Diagnosing Cartilage Damage In Vivo. Cartilage 2016; 7:39-51. [PMID: 26958316 PMCID: PMC4749750 DOI: 10.1177/1947603515602307] [Citation(s) in RCA: 23] [Impact Index Per Article: 2.9] [Reference Citation Analysis] [Abstract] [Key Words] [Track Full Text] [Download PDF] [Figures] [Journal Information] [Submit a Manuscript] [Subscribe] [Scholar Register] [Indexed: 12/23/2022] Open
Abstract
Advances in current clinical modalities, including magnetic resonance imaging and computed tomography, allow for earlier diagnoses of cartilage damage that could mitigate progression to osteoarthritis. However, current imaging modalities do not detect submicrometer damage. Developments in in vivo or arthroscopic techniques, including optical coherence tomography, ultrasonography, bioelectricity including streaming potential measurement, noninvasive electroarthrography, and multiphoton microscopy can detect damage at an earlier time point, but they are limited by a lack of penetration and the ability to assess an entire joint. This article reviews current advancements in clinical and developing modalities that can aid in the early diagnosis of cartilage injury and facilitate studies of interventional therapeutics.
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Affiliation(s)
| | | | - Matthew F. Koff
- MRI Laboratory, Hospital for Special Surgery, New York, NY, USA
| | | | | | - Lisa A. Fortier
- Department of Clinical Sciences, Cornell University, Ithaca, NY, USA,Lisa A. Fortier, Department of Clinical Sciences, Cornell University, VMC C3-181, Ithaca, NY 14853, USA. Email
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38
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Gilson RC, Tang R, Som A, Klajer C, Sarder P, Sudlow GP, Akers WJ, Achilefu S. Protonation and Trapping of a Small pH-Sensitive Near-Infrared Fluorescent Molecule in the Acidic Tumor Environment Delineate Diverse Tumors in Vivo. Mol Pharm 2015; 12:4237-46. [PMID: 26488921 DOI: 10.1021/acs.molpharmaceut.5b00430] [Citation(s) in RCA: 26] [Impact Index Per Article: 2.9] [Reference Citation Analysis] [Abstract] [Key Words] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Indexed: 12/11/2022]
Abstract
Enhanced glycolysis and poor perfusion in most solid malignant tumors create an acidic extracellular environment, which enhances tumor growth, invasion, and metastasis. Complex molecular systems have been explored for imaging and treating these tumors. Here, we report the development of a small molecule, LS662, that emits near-infrared (NIR) fluorescence upon protonation by the extracellular acidic pH environment of diverse solid tumors. Protonation of LS662 induces selective internalization into tumor cells and retention in the tumor microenvironment. Noninvasive NIR imaging demonstrates selective retention of the pH sensor in diverse tumors, and two-photon microscopy of ex vivo tumors reveals significant retention of LS662 in tumor cells and the acid tumor microenvironment. Passive and active internalization processes combine to enhance NIR fluorescence in tumors over time. The low background fluorescence allows tumors to be detected with high sensitivity, as well as dead or dying cells to be delineated from healthy cells. In addition to demonstrating the feasibility of using small molecule pH sensors to image multiple aggressive solid tumor types via a protonation-induced internalization and retention pathway, the study reveals the potential of using LS662 to monitor treatment response and tumor-targeted drug delivery.
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Affiliation(s)
- Rebecca C Gilson
- Departments of †Radiology, ‡Biomedical Engineering, and §Biochemistry & Molecular Biophysics, Washington University in St. Louis , St. Louis 63110, United States
| | - Rui Tang
- Departments of †Radiology, ‡Biomedical Engineering, and §Biochemistry & Molecular Biophysics, Washington University in St. Louis , St. Louis 63110, United States
| | - Avik Som
- Departments of †Radiology, ‡Biomedical Engineering, and §Biochemistry & Molecular Biophysics, Washington University in St. Louis , St. Louis 63110, United States
| | - Chloe Klajer
- Departments of †Radiology, ‡Biomedical Engineering, and §Biochemistry & Molecular Biophysics, Washington University in St. Louis , St. Louis 63110, United States
| | - Pinaki Sarder
- Departments of †Radiology, ‡Biomedical Engineering, and §Biochemistry & Molecular Biophysics, Washington University in St. Louis , St. Louis 63110, United States
| | - Gail P Sudlow
- Departments of †Radiology, ‡Biomedical Engineering, and §Biochemistry & Molecular Biophysics, Washington University in St. Louis , St. Louis 63110, United States
| | - Walter J Akers
- Departments of †Radiology, ‡Biomedical Engineering, and §Biochemistry & Molecular Biophysics, Washington University in St. Louis , St. Louis 63110, United States
| | - Samuel Achilefu
- Departments of †Radiology, ‡Biomedical Engineering, and §Biochemistry & Molecular Biophysics, Washington University in St. Louis , St. Louis 63110, United States
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39
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Abstract
Advancements in coherent Raman scattering (CRS) microscopy have enabled label-free visualization and analysis of functional, endogenous biomolecules in living systems. When compared with spontaneous Raman microscopy, a key advantage of CRS microscopy is the dramatic improvement in imaging speed, which gives rise to real-time vibrational imaging of live biological samples. Using molecular vibrational signatures, recently developed hyperspectral CRS microscopy has improved the readout of chemical information available from CRS images. In this article, we review recent achievements in CRS microscopy, focusing on the theory of the CRS signal-to-noise ratio, imaging speed, technical developments, and applications of CRS imaging in bioscience and clinical settings. In addition, we present possible future directions that the use of this technology may take.
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Affiliation(s)
- Chi Zhang
- Weldon School of Biomedical Engineering and Department of Chemistry, Purdue University, West Lafayette, Indiana 47907;
| | - Delong Zhang
- Weldon School of Biomedical Engineering and Department of Chemistry, Purdue University, West Lafayette, Indiana 47907;
| | - Ji-Xin Cheng
- Weldon School of Biomedical Engineering and Department of Chemistry, Purdue University, West Lafayette, Indiana 47907;
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40
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Endres BT, Staruschenko A, Schulte M, Geurts AM, Palygin O. Two-photon Imaging of Intracellular Ca2+ Handling and Nitric Oxide Production in Endothelial and Smooth Muscle Cells of an Isolated Rat Aorta. J Vis Exp 2015:e52734. [PMID: 26132549 DOI: 10.3791/52734] [Citation(s) in RCA: 3] [Impact Index Per Article: 0.3] [Reference Citation Analysis] [Abstract] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Indexed: 12/17/2022] Open
Abstract
Calcium is a very important regulator of many physiological processes in vascular tissues. Most endothelial and smooth muscle functions highly depend on changes in intracellular calcium ([Ca(2+)]i) and nitric oxide (NO). In order to understand how [Ca(2+)]i, NO and downstream molecules are handled by a blood vessel in response to vasoconstrictors and vasodilators, we developed a novel technique that applies calcium-labeling (or NO-labeling) dyes with two photon microscopy to measure calcium handling (or NO production) in isolated blood vessels. Described here is a detailed step-by-step procedure that demonstrates how to isolate an aorta from a rat, label calcium or NO within the endothelial or smooth muscle cells, and image calcium transients (or NO production) using a two photon microscope following physiological or pharmacological stimuli. The benefits of using the method are multi-fold: 1) it is possible to simultaneously measure calcium transients in both endothelial cells and smooth muscle cells in response to different stimuli; 2) it allows one to image endothelial cells and smooth muscle cells in their native setting; 3) this method is very sensitive to intracellular calcium or NO changes and generates high resolution images for precise measurements; and 4) described approach can be applied to the measurement of other molecules, such as reactive oxygen species. In summary, application of two photon laser emission microscopy to monitor calcium transients and NO production in the endothelial and smooth muscle cells of an isolated blood vessel has provided high quality quantitative data and promoted our understanding of the mechanisms regulating vascular function.
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Affiliation(s)
- Bradley T Endres
- Departments of Physiology, Medical College of Wisconsin; Human and Molecular Genetics Center, Medical College of Wisconsin
| | | | | | - Aron M Geurts
- Departments of Physiology, Medical College of Wisconsin; Human and Molecular Genetics Center, Medical College of Wisconsin; Cardiovascular Center, Medical College of Wisconsin
| | - Oleg Palygin
- Departments of Physiology, Medical College of Wisconsin
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41
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Chaudhary R, Campbell KR, Tilbury KB, Vanderby R, Block WF, Kijowski R, Campagnola PJ. Articular cartilage zonal differentiation via 3D Second-Harmonic Generation imaging microscopy. Connect Tissue Res 2015; 56:76-86. [PMID: 25738523 PMCID: PMC4497507 DOI: 10.3109/03008207.2015.1013192] [Citation(s) in RCA: 14] [Impact Index Per Article: 1.6] [Reference Citation Analysis] [Abstract] [Key Words] [Track Full Text] [Journal Information] [Submit a Manuscript] [Subscribe] [Scholar Register] [Indexed: 02/03/2023]
Abstract
PURPOSE The collagen structure throughout the patella has not been thoroughly investigated by 3D imaging, where the majority of the existing data come from histological cross sections. It is important to have a better understanding of the architecture in normal tissues, where this could then be applied to imaging of diseased states. METHODS To address this shortcoming, we investigated the combined use of collagen-specific Second-Harmonic Generation (SHG) imaging and measurement of bulk optical properties to characterize collagen fiber orientations of the histologically defined zones of bovine articular cartilage. Forward and backward SHG intensities of sections from superficial, middle and deep zones were collected as a function of depth and analyzed by Monte Carlo simulations to extract the SHG creation direction, which is related to the fibrillar assembly. RESULTS Our results revealed differences in SHG forward-backward response between the three zones, where these are consistent with a previously developed model of SHG emission. Some of the findings are consistent with that from other modalities; however, SHG analysis showed the middle zone had the most organized fibril assembly. While not distinct, we also report bulk optical property values for these different zones within the patella. CONCLUSIONS Collectively, these results provide quantitative measurements of structural changes at both the fiber and fibril assembly of the different cartilage zones and reveals structural information not possible by other microscope modalities. This can provide quantitative insight to the collagen fiber network in normal cartilage, which may ultimately be developed as a biomarker for osteoarthritis.
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Affiliation(s)
- Rajeev Chaudhary
- Department of Biomedical Engineering, University of Wisconsin-Madison, Madison, WI,Department of Orthopedics & Rehabilitation, University of Wisconsin-Madison, Madison, WI
| | - Kirby R. Campbell
- Department of Biomedical Engineering, University of Wisconsin-Madison, Madison, WI,Department of Laboratory for Optical and Computational Instrumentation, University of Wisconsin-Madison, Madison, WI
| | - Karissa B. Tilbury
- Department of Biomedical Engineering, University of Wisconsin-Madison, Madison, WI,Department of Laboratory for Optical and Computational Instrumentation, University of Wisconsin-Madison, Madison, WI
| | - Ray Vanderby
- Department of Biomedical Engineering, University of Wisconsin-Madison, Madison, WI,Department of Orthopedics & Rehabilitation, University of Wisconsin-Madison, Madison, WI
| | - Walter F. Block
- Department of Biomedical Engineering, University of Wisconsin-Madison, Madison, WI,Department of Medical Physics, University of Wisconsin-Madison, Madison, WI,Department of Radiology, University of Wisconsin-Madison, Madison, WI
| | - Richard Kijowski
- Department of Radiology, University of Wisconsin-Madison, Madison, WI
| | - Paul J. Campagnola
- Department of Biomedical Engineering, University of Wisconsin-Madison, Madison, WI,Department of Laboratory for Optical and Computational Instrumentation, University of Wisconsin-Madison, Madison, WI,Department of Medical Physics, University of Wisconsin-Madison, Madison, WI,Corresponding author:
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42
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Chow MJ, Turcotte R, Lin CP, Zhang Y. Arterial extracellular matrix: a mechanobiological study of the contributions and interactions of elastin and collagen. Biophys J 2015; 106:2684-92. [PMID: 24940786 DOI: 10.1016/j.bpj.2014.05.014] [Citation(s) in RCA: 134] [Impact Index Per Article: 14.9] [Reference Citation Analysis] [Abstract] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Received: 11/06/2013] [Revised: 03/04/2014] [Accepted: 05/05/2014] [Indexed: 01/01/2023] Open
Abstract
The complex network structure of elastin and collagen extracellular matrix (ECM) forms the primary load bearing components in the arterial wall. The structural and mechanobiological interactions between elastin and collagen are important for properly functioning arteries. Here, we examined the elastin and collagen organization, realignment, and recruitment by coupling mechanical loading and multiphoton imaging. Two-photon excitation fluorescence and second harmonic generation methods were performed with a multiphoton video-rate microscope to capture real time changes to the elastin and collagen structure during biaxial deformation. Enzymatic removal of elastin was performed to assess the structural changes of the remaining collagen structure. Quantitative analysis of the structural changes to elastin and collagen was made using a combination of two-dimensional fast Fourier transform and fractal analysis, which allows for a more complete understanding of structural changes. Our study provides new quantitative evidence, to our knowledge on the sequential engagement of different arterial ECM components in response to mechanical loading. The adventitial collagen exists as large wavy bundles of fibers that exhibit fiber engagement after 20% strain. The medial collagen is engaged throughout the stretching process, and prominent elastic fiber engagement is observed up to 20% strain after which the engagement plateaus. The fiber orientation distribution functions show remarkably different changes in the ECM structure in response to mechanical loading. The medial collagen shows an evident preferred circumferential distribution, however the fiber families of adventitial collagen are obscured by their waviness at no or low mechanical strains. Collagen fibers in both layers exhibit significant realignment in response to unequal biaxial loading. The elastic fibers are much more uniformly distributed and remained relatively unchanged due to loading. Removal of elastin produces similar structural changes in collagen as mechanical loading. Our study suggests that the elastic fibers are under tension and impart an intrinsic compressive stress on the collagen.
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Affiliation(s)
- Ming-Jay Chow
- Department of Mechanical Engineering, Boston University, Boston, Massachusetts
| | - Raphaël Turcotte
- Department of Biomedical Engineering, Boston University, Boston, Massachusetts; Center for Systems Biology, Advanced Microscopy Program, Wellman Center for Photomedicine, Massachusetts General Hospital, Harvard Medical School, Boston, Massachusetts
| | - Charles P Lin
- Center for Systems Biology, Advanced Microscopy Program, Wellman Center for Photomedicine, Massachusetts General Hospital, Harvard Medical School, Boston, Massachusetts
| | - Yanhang Zhang
- Department of Mechanical Engineering, Boston University, Boston, Massachusetts; Department of Biomedical Engineering, Boston University, Boston, Massachusetts.
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43
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Kiyomatsu H, Oshima Y, Saitou T, Miyazaki T, Hikita A, Miura H, Iimura T, Imamura T. Quantitative SHG imaging in osteoarthritis model mice, implying a diagnostic application. BIOMEDICAL OPTICS EXPRESS 2015; 6:405-20. [PMID: 25780732 PMCID: PMC4354585 DOI: 10.1364/boe.6.000405] [Citation(s) in RCA: 20] [Impact Index Per Article: 2.2] [Reference Citation Analysis] [Abstract] [Key Words] [Track Full Text] [Subscribe] [Scholar Register] [Received: 11/10/2014] [Revised: 12/23/2014] [Accepted: 12/29/2014] [Indexed: 05/28/2023]
Abstract
Osteoarthritis (OA) restricts the daily activities of patients and significantly decreases their quality of life. The development of non-invasive quantitative methods for properly diagnosing and evaluating the process of degeneration of articular cartilage due to OA is essential. Second harmonic generation (SHG) imaging enables the observation of collagen fibrils in live tissues or organs without staining. In the present study, we employed SHG imaging of the articular cartilage in OA model mice ex vivo. Consequently, three-dimensional SHG imaging with successive image processing and statistical analyses allowed us to successfully characterize histopathological changes in the articular cartilage consistently confirmed on histological analyses. The quantitative SHG imaging technique presented in this study constitutes a diagnostic application of this technology in the setting of OA.
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Affiliation(s)
- Hiroshi Kiyomatsu
- Department of Orthopedic Surgery, Graduate School of Medicine, Ehime University Shitukawa Toon city, Ehime, 791-0295,
Japan
- Molecular Medicine for Pathogenesis, Graduate School of Medicine, Ehime University, Shitukawa Toon city, Ehime, 791-0295,
Japan
- Artificial Joint Integrated Center, Ehime University Hospital, Shitukawa Toon city, Ehime, 791-0295,
Japan
| | - Yusuke Oshima
- Molecular Medicine for Pathogenesis, Graduate School of Medicine, Ehime University, Shitukawa Toon city, Ehime, 791-0295,
Japan
- Translational Research Center, Ehime University Hospital, Shitukawa Toon city, Ehime, 791-0295,
Japan
- Core Research for Evolutional Science and Technology, Shitukawa Toon city, Ehime, 791-0295,
Japan
- Division of Bio-Imaging, Proteo-Science Center, Ehime University, Shitukawa Toon city, Ehime, 791-0295,
Japan
| | - Takashi Saitou
- Molecular Medicine for Pathogenesis, Graduate School of Medicine, Ehime University, Shitukawa Toon city, Ehime, 791-0295,
Japan
- Artificial Joint Integrated Center, Ehime University Hospital, Shitukawa Toon city, Ehime, 791-0295,
Japan
| | - Tsuyoshi Miyazaki
- Department of Orthopaedic Surgery, Tokyo Metropolitan Geriatric Hospital and Institute of Gerontology, 35-2, Sakaecho, Itabashi-ku, Tokyo, 173-0015,
Japan
| | - Atsuhiko Hikita
- Molecular Medicine for Pathogenesis, Graduate School of Medicine, Ehime University, Shitukawa Toon city, Ehime, 791-0295,
Japan
- Core Research for Evolutional Science and Technology, Shitukawa Toon city, Ehime, 791-0295,
Japan
- Division of Bio-Imaging, Proteo-Science Center, Ehime University, Shitukawa Toon city, Ehime, 791-0295,
Japan
| | - Hiromasa Miura
- Department of Orthopedic Surgery, Graduate School of Medicine, Ehime University Shitukawa Toon city, Ehime, 791-0295,
Japan
- Artificial Joint Integrated Center, Ehime University Hospital, Shitukawa Toon city, Ehime, 791-0295,
Japan
- Translational Research Center, Ehime University Hospital, Shitukawa Toon city, Ehime, 791-0295,
Japan
| | - Tadahiro Iimura
- Artificial Joint Integrated Center, Ehime University Hospital, Shitukawa Toon city, Ehime, 791-0295,
Japan
- Translational Research Center, Ehime University Hospital, Shitukawa Toon city, Ehime, 791-0295,
Japan
- Core Research for Evolutional Science and Technology, Shitukawa Toon city, Ehime, 791-0295,
Japan
- Division of Bio-Imaging, Proteo-Science Center, Ehime University, Shitukawa Toon city, Ehime, 791-0295,
Japan
| | - Takeshi Imamura
- Molecular Medicine for Pathogenesis, Graduate School of Medicine, Ehime University, Shitukawa Toon city, Ehime, 791-0295,
Japan
- Artificial Joint Integrated Center, Ehime University Hospital, Shitukawa Toon city, Ehime, 791-0295,
Japan
- Translational Research Center, Ehime University Hospital, Shitukawa Toon city, Ehime, 791-0295,
Japan
- Core Research for Evolutional Science and Technology, Shitukawa Toon city, Ehime, 791-0295,
Japan
- Division of Bio-Imaging, Proteo-Science Center, Ehime University, Shitukawa Toon city, Ehime, 791-0295,
Japan
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44
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Bell JS, Christmas J, Mansfield JC, Everson RM, Winlove CP. Micromechanical response of articular cartilage to tensile load measured using nonlinear microscopy. Acta Biomater 2014; 10:2574-81. [PMID: 24525036 DOI: 10.1016/j.actbio.2014.02.008] [Citation(s) in RCA: 17] [Impact Index Per Article: 1.7] [Reference Citation Analysis] [Abstract] [Key Words] [MESH Headings] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Received: 08/20/2013] [Revised: 01/21/2014] [Accepted: 02/03/2014] [Indexed: 11/28/2022]
Abstract
Articular cartilage (AC) is a highly anisotropic biomaterial, and its complex mechanical properties have been a topic of intense investigation for over 60 years. Recent advances in the field of nonlinear optics allow the individual constituents of AC to be imaged in living tissue without the need for exogenous contrast agents. Combining mechanical testing with nonlinear microscopy provides a wealth of information about microscopic responses to load. This work investigates the inhomogeneous distribution of strain in loaded AC by tracking the movement and morphological changes of individual chondrocytes using point pattern matching and Bayesian modeling. This information can be used to inform models of mechanotransduction and pathogenesis, and is readily extendable to various other connective tissues.
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Affiliation(s)
- J S Bell
- Department of Physics, University of Exeter, Stocker Road, Exeter EX4 4QL, UK.
| | - J Christmas
- Department of Computer Science, University of Exeter, North Park Road, Exeter EX4 4QF, UK
| | - J C Mansfield
- Department of Physics, University of Exeter, Stocker Road, Exeter EX4 4QL, UK
| | - R M Everson
- Department of Computer Science, University of Exeter, North Park Road, Exeter EX4 4QF, UK
| | - C P Winlove
- Department of Physics, University of Exeter, Stocker Road, Exeter EX4 4QL, UK
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45
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Green EM, Mansfield JC, Bell JS, Winlove CP. The structure and micromechanics of elastic tissue. Interface Focus 2014; 4:20130058. [PMID: 24748954 PMCID: PMC3982448 DOI: 10.1098/rsfs.2013.0058] [Citation(s) in RCA: 73] [Impact Index Per Article: 7.3] [Reference Citation Analysis] [Abstract] [Key Words] [Grants] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Indexed: 12/22/2022] Open
Abstract
Elastin is a major component of tissues such as lung and blood vessels, and endows them with the long-range elasticity necessary for their physiological functions. Recent research has revealed the complexity of these elastin structures and drawn attention to the existence of extensive networks of fine elastin fibres in tissues such as articular cartilage and the intervertebral disc. Nonlinear microscopy, allowing the visualization of these structures in living tissues, is informing analysis of their mechanical properties. Elastic fibres are complex in composition and structure containing, in addition to elastin, an array of microfibrillar proteins, principally fibrillin. Raman microspectrometry and X-ray scattering have provided new insights into the mechanisms of elasticity of the individual component proteins at the molecular and fibrillar levels, but more remains to be done in understanding their mechanical interactions in composite matrices. Elastic tissue is one of the most stable components of the extracellular matrix, but impaired mechanical function is associated with ageing and diseases such as atherosclerosis and diabetes. Efforts to understand these associations through studying the effects of processes such as calcium and lipid binding and glycation on the mechanical properties of elastin preparations in vitro have produced a confusing picture, and further efforts are required to determine the molecular basis of such effects.
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Affiliation(s)
| | | | | | - C. Peter Winlove
- Department of Physics, College of Engineering Mathematics and Physical Science, University of Exeter, Stocker Road, Exeter EX4 4QL, UK
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46
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He B, Wu JP, Kirk TB, Carrino JA, Xiang C, Xu J. High-resolution measurements of the multilayer ultra-structure of articular cartilage and their translational potential. Arthritis Res Ther 2014; 16:205. [PMID: 24946278 PMCID: PMC4061724 DOI: 10.1186/ar4506] [Citation(s) in RCA: 40] [Impact Index Per Article: 4.0] [Reference Citation Analysis] [Abstract] [Download PDF] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Indexed: 11/16/2022] Open
Abstract
Current musculoskeletal imaging techniques usually target the macro-morphology of
articular cartilage or use histological analysis. These techniques are able to reveal
advanced osteoarthritic changes in articular cartilage but fail to give detailed
information to distinguish early osteoarthritis from healthy cartilage, and this
necessitates high-resolution imaging techniques measuring cells and the extracellular
matrix within the multilayer structure of articular cartilage. This review provides a
comprehensive exploration of the cellular components and extracellular matrix of
articular cartilage as well as high-resolution imaging techniques, including magnetic
resonance image, electron microscopy, confocal laser scanning microscopy, second
harmonic generation microscopy, and laser scanning confocal arthroscopy, in the
measurement of multilayer ultra-structures of articular cartilage. This review also
provides an overview for micro-structural analysis of the main components of normal
or osteoarthritic cartilage and discusses the potential and challenges associated
with developing non-invasive high-resolution imaging techniques for both research and
clinical diagnosis of early to late osteoarthritis.
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47
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Nimeskern L, van Osch GJ, Müller R, Stok KS. Quantitative Evaluation of Mechanical Properties in Tissue-Engineered Auricular Cartilage. TISSUE ENGINEERING PART B-REVIEWS 2014; 20:17-27. [DOI: 10.1089/ten.teb.2013.0117] [Citation(s) in RCA: 28] [Impact Index Per Article: 2.8] [Reference Citation Analysis] [Track Full Text] [Subscribe] [Scholar Register] [Indexed: 01/01/2023]
Affiliation(s)
- Luc Nimeskern
- Institute for Biomechanics, ETH Zurich, Zurich, Switzerland
| | - Gerjo J.V.M. van Osch
- Departments of Otorhinolaryngology and Orthopaedics, Erasmus MC, University Medical Center Rotterdam, Rotterdam, The Netherlands
| | - Ralph Müller
- Institute for Biomechanics, ETH Zurich, Zurich, Switzerland
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48
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Duan X, Wu J, Swift B, Kirk TB. Texture analysis of the 3D collagen network and automatic classification of the physiology of articular cartilage. Comput Methods Biomech Biomed Engin 2014; 18:931-943. [DOI: 10.1080/10255842.2013.864284] [Citation(s) in RCA: 4] [Impact Index Per Article: 0.4] [Reference Citation Analysis] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Indexed: 10/25/2022]
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49
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Jutila AA, Zignego DL, Hwang BK, Hilmer JK, Hamerly T, Minor CA, Walk ST, June RK. Candidate mediators of chondrocyte mechanotransduction via targeted and untargeted metabolomic measurements. Arch Biochem Biophys 2014; 545:116-23. [PMID: 24440608 DOI: 10.1016/j.abb.2014.01.011] [Citation(s) in RCA: 28] [Impact Index Per Article: 2.8] [Reference Citation Analysis] [Abstract] [Key Words] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Received: 10/10/2013] [Revised: 01/10/2014] [Accepted: 01/11/2014] [Indexed: 11/30/2022]
Abstract
Chondrocyte mechanotransduction is the process by which cartilage cells transduce mechanical loads into biochemical and biological signals. Previous studies have identified several pathways by which chondrocytes transduce mechanical loads, yet a general understanding of which signals are activated and in what order remains elusive. This study was performed to identify candidate mediators of chondrocyte mechanotransduction using SW1353 chondrocytes embedded in physiologically stiff agarose. Dynamic compression was applied to cell-seeded constructs for 0-30min, followed immediately by whole-cell metabolite extraction. Metabolites were detected via LC-MS, and compounds of interest were identified via database searches. We found several metabolites which were statistically different between the experimental groups, and we report the detection of 5 molecules which are not found in metabolite databases of known compounds indicating potential novel molecules. Targeted studies to quantify the response of central energy metabolites to compression found a transient increase in the ratio of NADP+ to NADPH and a continual decrease in the ratio of GDP to GTP, suggesting a flux of energy into the TCA cycle. These data are consistent with the remodeling of cytoskeletal components by mechanically induced signaling, and add substantial new data to a complex picture of how chondrocytes transduce mechanical loads.
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Affiliation(s)
- Aaron A Jutila
- Department of Mechanical and Industrial Engineering, Montana State University, PO Box 173800, Bozeman, MT 59717-3800, United States
| | - Donald L Zignego
- Department of Mechanical and Industrial Engineering, Montana State University, PO Box 173800, Bozeman, MT 59717-3800, United States
| | - Bradley K Hwang
- Department of Mechanical and Industrial Engineering, Montana State University, PO Box 173800, Bozeman, MT 59717-3800, United States
| | - Jonathan K Hilmer
- Department of Chemistry and Biochemistry, Montana State University, PO Box 173800, Bozeman, MT 59717-3800, United States
| | - Timothy Hamerly
- Department of Chemistry and Biochemistry, Montana State University, PO Box 173800, Bozeman, MT 59717-3800, United States
| | - Cody A Minor
- Department of Mechanical and Industrial Engineering, Montana State University, PO Box 173800, Bozeman, MT 59717-3800, United States
| | - Seth T Walk
- Department of Immunology and Microbiology, Montana State University, PO Box 173800, Bozeman, MT 59717-3800, United States
| | - Ronald K June
- Department of Cell Biology and Neuroscience, Montana State University, PO Box 173800, Bozeman, MT 59717-3800, United States.
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Alkhouli N, Mansfield J, Green E, Bell J, Knight B, Liversedge N, Tham JC, Welbourn R, Shore AC, Kos K, Winlove CP. The mechanical properties of human adipose tissues and their relationships to the structure and composition of the extracellular matrix. Am J Physiol Endocrinol Metab 2013; 305:E1427-35. [PMID: 24105412 DOI: 10.1152/ajpendo.00111.2013] [Citation(s) in RCA: 145] [Impact Index Per Article: 13.2] [Reference Citation Analysis] [Abstract] [Key Words] [MESH Headings] [Track Full Text] [Journal Information] [Submit a Manuscript] [Subscribe] [Scholar Register] [Indexed: 12/15/2022]
Abstract
Adipose tissue (AT) expansion in obesity is characterized by cellular growth and continuous extracellular matrix (ECM) remodeling with increased fibrillar collagen deposition. It is hypothesized that the matrix can inhibit cellular expansion and lipid storage. Therefore, it is important to fully characterize the ECM's biomechanical properties and its interactions with cells. In this study, we characterize and compare the mechanical properties of human subcutaneous and omental tissues, which have different physiological functions. AT was obtained from 44 subjects undergoing surgery. Force/extension and stress/relaxation data were obtained. The effects of osmotic challenge were measured to investigate the cellular contribution to tissue mechanics. Tissue structure and its response to tensile strain were determined using nonlinear microscopy. AT showed nonlinear stress/strain characteristics of up to a 30% strain. Comparing paired subcutaneous and omental samples (n = 19), the moduli were lower in subcutaneous: initial 1.6 ± 0.8 (means ± SD) and 2.9 ± 1.5 kPa (P = 0.001), final 11.7 ± 6.4 and 32 ± 15.6 kPa (P < 0.001), respectively. The energy dissipation density was lower in subcutaneous AT (n = 13): 0.1 ± 0.1 and 0.3 ± 0.2 kPa, respectively (P = 0.006). Stress/relaxation followed a two-exponential time course. When the incubation medium was exchanged for deionized water in specimens held at 30% strain, force decreased by 31%, and the final modulus increased significantly. Nonlinear microscopy revealed collagen and elastin networks in close proximity to adipocytes and a larger-scale network of larger fiber bundles. There was considerable microscale heterogeneity in the response to strain in both cells and matrix fibers. These results suggest that subcutaneous AT has greater capacity for expansion and recovery from mechanical deformation than omental AT.
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Affiliation(s)
- Nadia Alkhouli
- Obesity Research Group, Institute of Biomedical and Clinical Science, University of Exeter Medical School, University of Exeter, Exeter, United Kingdom
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