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Nanes BA, Bhatt K, Azarova E, Rajendran D, Munawar S, Isogai T, Dean KM, Danuser G. Shifts in keratin isoform expression activate motility signals during wound healing. Dev Cell 2024:S1534-5807(24)00389-7. [PMID: 39002537 DOI: 10.1016/j.devcel.2024.06.011] [Citation(s) in RCA: 0] [Impact Index Per Article: 0] [Reference Citation Analysis] [Abstract] [Key Words] [Grants] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Received: 06/09/2023] [Revised: 04/15/2024] [Accepted: 06/17/2024] [Indexed: 07/15/2024]
Abstract
Keratin intermediate filaments confer structural stability to epithelial tissues, but the reason this simple mechanical function requires a protein family with 54 isoforms is not understood. During skin wound healing, a shift in keratin isoform expression alters the composition of keratin filaments. If and how this change modulates cellular functions that support epidermal remodeling remains unclear. We report an unexpected effect of keratin isoform variation on kinase signal transduction. Increased expression of wound-associated keratin 6A, but not of steady-state keratin 5, potentiated keratinocyte migration and wound closure without compromising mechanical stability by activating myosin motors to increase contractile force generation. These results substantially expand the functional repertoire of intermediate filaments from their canonical role as mechanical scaffolds to include roles as isoform-tuned signaling scaffolds that organize signal transduction cascades in space and time to influence epithelial cell state.
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Affiliation(s)
- Benjamin A Nanes
- Department of Dermatology, UT Southwestern Medical Center, Dallas, TX 75390, USA; Lyda Hill Department of Bioinformatics and Cecil H and Ida Green Center for Systems Biology, UT Southwestern Medical Center, Dallas, TX 75390, USA.
| | - Kushal Bhatt
- Lyda Hill Department of Bioinformatics and Cecil H and Ida Green Center for Systems Biology, UT Southwestern Medical Center, Dallas, TX 75390, USA
| | - Evgenia Azarova
- Lyda Hill Department of Bioinformatics and Cecil H and Ida Green Center for Systems Biology, UT Southwestern Medical Center, Dallas, TX 75390, USA
| | - Divya Rajendran
- Lyda Hill Department of Bioinformatics and Cecil H and Ida Green Center for Systems Biology, UT Southwestern Medical Center, Dallas, TX 75390, USA
| | - Sabahat Munawar
- Lyda Hill Department of Bioinformatics and Cecil H and Ida Green Center for Systems Biology, UT Southwestern Medical Center, Dallas, TX 75390, USA
| | - Tadamoto Isogai
- Lyda Hill Department of Bioinformatics and Cecil H and Ida Green Center for Systems Biology, UT Southwestern Medical Center, Dallas, TX 75390, USA
| | - Kevin M Dean
- Lyda Hill Department of Bioinformatics and Cecil H and Ida Green Center for Systems Biology, UT Southwestern Medical Center, Dallas, TX 75390, USA
| | - Gaudenz Danuser
- Lyda Hill Department of Bioinformatics and Cecil H and Ida Green Center for Systems Biology, UT Southwestern Medical Center, Dallas, TX 75390, USA.
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2
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Nanes BA, Bhatt K, Boujemaa-Paterski R, Azarova E, Munawar S, Rajendran D, Isogai T, Dean KM, Medalia O, Danuser G. Keratin isoform shifts modulate motility signals during wound healing. BIORXIV : THE PREPRINT SERVER FOR BIOLOGY 2024:2023.05.04.538989. [PMID: 37205459 PMCID: PMC10187270 DOI: 10.1101/2023.05.04.538989] [Citation(s) in RCA: 0] [Impact Index Per Article: 0] [Reference Citation Analysis] [Abstract] [Grants] [Track Full Text] [Subscribe] [Scholar Register] [Indexed: 05/21/2023]
Abstract
Keratin intermediate filaments form strong mechanical scaffolds that confer structural stability to epithelial tissues, but the reason this function requires a protein family with 54 isoforms is not understood. During skin wound healing, a shift in keratin isoform expression alters the composition of keratin filaments. How this change modulates cellular function to support epidermal remodeling remains unclear. We report an unexpected effect of keratin isoform variation on kinase signal transduction. Increased expression of wound-associated keratin 6A, but not of steady-state keratin 5, potentiated keratinocyte migration and wound closure without compromising epidermal stability by activating myosin motors. This pathway depended on isoform-specific interaction between intrinsically disordered keratin head domains and non-filamentous vimentin shuttling myosin-activating kinases. These results substantially expand the functional repertoire of intermediate filaments from their canonical role as mechanical scaffolds to include roles as isoform-tuned signaling scaffolds that organize signal transduction cascades in space and time to influence epithelial cell state.
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Affiliation(s)
- Benjamin A Nanes
- Department of Dermatology, UT Southwestern Medical Center; Dallas, TX 75390, USA
- Lyda Hill Department of Bioinformatics and Cecil H and Ida Green Center for Systems Biology, UT Southwestern Medical Center; Dallas, TX 75390, USA
| | - Kushal Bhatt
- Lyda Hill Department of Bioinformatics and Cecil H and Ida Green Center for Systems Biology, UT Southwestern Medical Center; Dallas, TX 75390, USA
| | | | - Evgenia Azarova
- Lyda Hill Department of Bioinformatics and Cecil H and Ida Green Center for Systems Biology, UT Southwestern Medical Center; Dallas, TX 75390, USA
- Present address: Department of Materials Science and Engineering, Johns Hopkins University; Baltimore, MD 21218, USA
| | - Sabahat Munawar
- Lyda Hill Department of Bioinformatics and Cecil H and Ida Green Center for Systems Biology, UT Southwestern Medical Center; Dallas, TX 75390, USA
| | - Divya Rajendran
- Lyda Hill Department of Bioinformatics and Cecil H and Ida Green Center for Systems Biology, UT Southwestern Medical Center; Dallas, TX 75390, USA
| | - Tadamoto Isogai
- Lyda Hill Department of Bioinformatics and Cecil H and Ida Green Center for Systems Biology, UT Southwestern Medical Center; Dallas, TX 75390, USA
| | - Kevin M Dean
- Lyda Hill Department of Bioinformatics and Cecil H and Ida Green Center for Systems Biology, UT Southwestern Medical Center; Dallas, TX 75390, USA
| | - Ohad Medalia
- Department of Biochemistry, University of Zurich; Zurich CH-8057, Switzerland
| | - Gaudenz Danuser
- Lyda Hill Department of Bioinformatics and Cecil H and Ida Green Center for Systems Biology, UT Southwestern Medical Center; Dallas, TX 75390, USA
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3
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Mittal N, Michels EB, Massey AE, Qiu Y, Royer-Weeden SP, Smith BR, Cartagena-Rivera AX, Han SJ. Myosin-independent stiffness sensing by fibroblasts is regulated by the viscoelasticity of flowing actin. COMMUNICATIONS MATERIALS 2024; 5:6. [PMID: 38741699 PMCID: PMC11090405 DOI: 10.1038/s43246-024-00444-0] [Citation(s) in RCA: 1] [Impact Index Per Article: 1.0] [Reference Citation Analysis] [Abstract] [Track Full Text] [Figures] [Subscribe] [Scholar Register] [Received: 06/01/2023] [Accepted: 01/02/2024] [Indexed: 05/16/2024]
Abstract
The stiffness of the extracellular matrix induces differential tension within integrin-based adhesions, triggering differential mechanoresponses. However, it has been unclear if the stiffness-dependent differential tension is induced solely by myosin activity. Here, we report that in the absence of myosin contractility, 3T3 fibroblasts still transmit stiffness-dependent differential levels of traction. This myosin-independent differential traction is regulated by polymerizing actin assisted by actin nucleators Arp2/3 and formin where formin has a stronger contribution than Arp2/3 to both traction and actin flow. Intriguingly, despite only slight changes in F-actin flow speed observed in cells with the combined inhibition of Arp2/3 and myosin compared to cells with sole myosin inhibition, they show a 4-times reduction in traction than cells with myosin-only inhibition. Our analyses indicate that traditional models based on rigid F-actin are inadequate for capturing such dramatic force reduction with similar actin flow. Instead, incorporating the F-actin network's viscoelastic properties is crucial. Our new model including the F-actin viscoelasticity reveals that Arp2/3 and formin enhance stiffness sensitivity by mechanically reinforcing the F-actin network, thereby facilitating more effective transmission of flow-induced forces. This model is validated by cell stiffness measurement with atomic force microscopy and experimental observation of model-predicted stiffness-dependent actin flow fluctuation.
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Affiliation(s)
- Nikhil Mittal
- Department of Biomedical Engineering, Michigan Technological University, Houghton, MI, USA
- Health Research Institute, Michigan Technological University, Houghton, MI, USA
| | - Etienne B. Michels
- Department of Biomedical Engineering, Michigan Technological University, Houghton, MI, USA
| | - Andrew E. Massey
- Section on Mechanobiology, National Institute of Biomedical Imaging and Bioengineering, National Institutes of Health, Bethesda, MD, USA
| | - Yunxiu Qiu
- Department of Biomedical Engineering, Michigan State University, Lansing, MI, USA
| | - Shaina P. Royer-Weeden
- Department of Biomedical Engineering, Michigan Technological University, Houghton, MI, USA
| | - Bryan R. Smith
- Department of Biomedical Engineering, Michigan State University, Lansing, MI, USA
| | - Alexander X. Cartagena-Rivera
- Section on Mechanobiology, National Institute of Biomedical Imaging and Bioengineering, National Institutes of Health, Bethesda, MD, USA
| | - Sangyoon J. Han
- Department of Biomedical Engineering, Michigan Technological University, Houghton, MI, USA
- Health Research Institute, Michigan Technological University, Houghton, MI, USA
- Department of Mechanical Engineering and Engineering Mechanics, Michigan Technological University, Houghton, MI, USA
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4
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Delanoë-Ayari H, Hiraiwa T, Marcq P, Rieu JP, Saw TB. 2.5D Traction Force Microscopy: Imaging three-dimensional cell forces at interfaces and biological applications. Int J Biochem Cell Biol 2023; 161:106432. [PMID: 37290687 DOI: 10.1016/j.biocel.2023.106432] [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: 12/25/2022] [Revised: 05/30/2023] [Accepted: 06/04/2023] [Indexed: 06/10/2023]
Abstract
The forces that cells, tissues, and organisms exert on the surface of a soft substrate can be measured using Traction Force Microscopy (TFM), an important and well-established technique in Mechanobiology. The usual TFM technique (two-dimensional, 2D TFM) treats only the in-plane component of the traction forces and omits the out-of-plane forces at the substrate interfaces (2.5D) that turn out to be important in many biological processes such as tissue migration and tumour invasion. Here, we review the imaging, material, and analytical tools to perform "2.5D TFM" and explain how they are different from 2D TFM. Challenges in 2.5D TFM arise primarily from the need to work with a lower imaging resolution in the z-direction, track fiducial markers in three-dimensions, and reliably and efficiently reconstruct mechanical stress from substrate deformation fields. We also discuss how 2.5D TFM can be used to image, map, and understand the complete force vectors in various important biological events of various length-scales happening at two-dimensional interfaces, including focal adhesions forces, cell diapedesis across tissue monolayers, the formation of three-dimensional tissue structures, and the locomotion of large multicellular organisms. We close with future perspectives including the use of new materials, imaging and machine learning techniques to continuously improve the 2.5D TFM in terms of imaging resolution, speed, and faithfulness of the force reconstruction procedure.
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Affiliation(s)
- Hélène Delanoë-Ayari
- University of Lyon, Université Claude Bernard Lyon 1, CNRS, Institut Lumière Matière, F-69622 Villeurbanne, France.
| | - Tetsuya Hiraiwa
- Mechanobiology Institute, National University of Singapore, Singapore; Institute of Physics, Academia Sinica, Taipei, Taiwan.
| | - Philippe Marcq
- Laboratoire Physique et Mécanique des Milieux Hétérogènes, Sorbonne Université, CNRS UMR 7636, ESPCI, Université Paris Cité, Paris, France.
| | - Jean-Paul Rieu
- University of Lyon, Université Claude Bernard Lyon 1, CNRS, Institut Lumière Matière, F-69622 Villeurbanne, France.
| | - Thuan Beng Saw
- Westlake Laboratory of Life Sciences and Biomedicine, Hangzhou, Zhejiang, China; School of Life Sciences, Westlake University, Hangzhou, Zhejiang, China.
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5
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The explorations of dynamic interactions of paxillin at the focal adhesions. BIOCHIMICA ET BIOPHYSICA ACTA. PROTEINS AND PROTEOMICS 2022; 1870:140825. [PMID: 35926716 DOI: 10.1016/j.bbapap.2022.140825] [Citation(s) in RCA: 0] [Impact Index Per Article: 0] [Reference Citation Analysis] [Abstract] [Key Words] [Track Full Text] [Subscribe] [Scholar Register] [Received: 01/11/2022] [Revised: 07/16/2022] [Accepted: 07/27/2022] [Indexed: 11/20/2022]
Abstract
Paxillin is one of the most important adapters in integrin-mediated adhesions that performs numerous crucial functions relying on its dynamic interactions. Its structural behavior serves different purposes, providing a base for several activities. The various domains of paxillin display different functions in the whole process of cell movements and have a significant role in cell adhesion, migration, signal transmission, and protein-protein interactions. On the other hand, some paxillin-associated proteins provide a unique spatiotemporal mechanism for regulating its dynamic characteristics in the tissue homeostasis and make it a more complex and decisive protein at the focal adhesions. This review briefly describes the structural adaptations and molecular mechanisms of recruitment of paxillin into adhesions, explains paxillin's binding dynamics and impact on adhesion stability and turnover, and reveals a variety of paxillin-associated regulatory mechanisms and how paxillin is embedded into the signaling networks.
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Grimm E, van der Hoeven F, Sardella D, Willig KI, Engel U, Veits N, Engel R, Cavalcanti-Adam EA, Bestvater F, Bordoni L, Jennemann R, Schönig K, Schiessl IM, Sandhoff R. A Clathrin light chain A reporter mouse for in vivo imaging of endocytosis. PLoS One 2022; 17:e0273660. [PMID: 36149863 PMCID: PMC9506643 DOI: 10.1371/journal.pone.0273660] [Citation(s) in RCA: 0] [Impact Index Per Article: 0] [Reference Citation Analysis] [Abstract] [MESH Headings] [Grants] [Track Full Text] [Download PDF] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Received: 12/16/2021] [Accepted: 08/13/2022] [Indexed: 11/20/2022] Open
Abstract
Clathrin-mediated endocytosis (CME) is one of the best studied cellular uptake pathways and its contributions to nutrient uptake, receptor signaling, and maintenance of the lipid membrane homeostasis have been already elucidated. Today, we still have a lack of understanding how the different components of this pathway cooperate dynamically in vivo. Therefore, we generated a reporter mouse model for CME by fusing eGFP endogenously in frame to clathrin light chain a (Clta) to track endocytosis in living mice. The fusion protein is expressed in all tissues, but in a cell specific manner, and can be visualized using fluorescence microscopy. Recruitment to nanobeads recorded by TIRF microscopy validated the functionality of the Clta-eGFP reporter. With this reporter model we were able to track the dynamics of Alexa594-BSA uptake in kidneys of anesthetized mice using intravital 2-photon microscopy. This reporter mouse model is not only a suitable and powerful tool to track CME in vivo in genetic or disease mouse models it can also help to shed light into the differential roles of the two clathrin light chain isoforms in health and disease.
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Affiliation(s)
- Elisabeth Grimm
- Lipid Pathobiochemistry Group, German Cancer Research Center (DKFZ), Heidelberg, Germany
- Faculty of Biosciences, Heidelberg University, Heidelberg, Germany
- * E-mail: (EG); (RS)
| | | | - Donato Sardella
- Department of Biomedicine, Aarhus University, Aarhus, Denmark
| | - Katrin I. Willig
- Optical Nanoscopy in Neuroscience, Center for Nanoscale Microscopy and Molecular Physiology of the Brain, University Medical Center Göttingen, Göttingen, Germany
- Max Planck Institute of Experimental Medicine, Goettingen, Germany
| | - Ulrike Engel
- Faculty of Biosciences, Heidelberg University, Heidelberg, Germany
- Nikon Imaging Center at Heidelberg University and Centre of Organismal Studies (COS), Bioquant, Heidelberg, Germany
| | - Nisha Veits
- Department of Cellular Biophysics, Max Planck Institute for Medical Research, Heidelberg, Germany
| | - Robert Engel
- Lipid Pathobiochemistry Group, German Cancer Research Center (DKFZ), Heidelberg, Germany
- Faculty of Biosciences, Heidelberg University, Heidelberg, Germany
| | | | - Felix Bestvater
- Light Microscopy Core Facility, German Cancer Research Center (DKFZ), Heidelberg, Germany
| | - Luca Bordoni
- Department of Biomedicine, Aarhus University, Aarhus, Denmark
| | - Richard Jennemann
- Lipid Pathobiochemistry Group, German Cancer Research Center (DKFZ), Heidelberg, Germany
| | - Kai Schönig
- Department of Molecular Biology, Central Institute of Mental Health, Mannheim, Germany
| | | | - Roger Sandhoff
- Lipid Pathobiochemistry Group, German Cancer Research Center (DKFZ), Heidelberg, Germany
- * E-mail: (EG); (RS)
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7
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Guo T, He C, Venado A, Zhou Y. Extracellular Matrix Stiffness in Lung Health and Disease. Compr Physiol 2022; 12:3523-3558. [PMID: 35766837 PMCID: PMC10088466 DOI: 10.1002/cphy.c210032] [Citation(s) in RCA: 5] [Impact Index Per Article: 2.5] [Reference Citation Analysis] [Abstract] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Indexed: 11/11/2022]
Abstract
The extracellular matrix (ECM) provides structural support and imparts a wide variety of environmental cues to cells. In the past decade, a growing body of work revealed that the mechanical properties of the ECM, commonly known as matrix stiffness, regulate the fundamental cellular processes of the lung. There is growing appreciation that mechanical interplays between cells and associated ECM are essential to maintain lung homeostasis. Dysregulation of ECM-derived mechanical signaling via altered mechanosensing and mechanotransduction pathways is associated with many common lung diseases. Matrix stiffening is a hallmark of lung fibrosis. The stiffened ECM is not merely a sequelae of lung fibrosis but can actively drive the progression of fibrotic lung disease. In this article, we provide a comprehensive view on the role of matrix stiffness in lung health and disease. We begin by summarizing the effects of matrix stiffness on the function and behavior of various lung cell types and on regulation of biomolecule activity and key physiological processes, including host immune response and cellular metabolism. We discuss the potential mechanisms by which cells probe matrix stiffness and convert mechanical signals to regulate gene expression. We highlight the factors that govern matrix stiffness and outline the role of matrix stiffness in lung development and the pathogenesis of pulmonary fibrosis, pulmonary hypertension, asthma, chronic obstructive pulmonary disease (COPD), and lung cancer. We envision targeting of deleterious matrix mechanical cues for treatment of fibrotic lung disease. Advances in technologies for matrix stiffness measurements and design of stiffness-tunable matrix substrates are also explored. © 2022 American Physiological Society. Compr Physiol 12:3523-3558, 2022.
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Affiliation(s)
- Ting Guo
- Division of Pulmonary, Allergy and Critical Care Medicine, Department of Medicine, University of Alabama at Birmingham, Alabama, USA.,Department of Respiratory Medicine, the Second Xiangya Hospital, Central-South University, Changsha, Hunan, China
| | - Chao He
- Division of Pulmonary, Allergy and Critical Care Medicine, Department of Medicine, University of Alabama at Birmingham, Alabama, USA
| | - Aida Venado
- Pulmonary, Critical Care, Allergy and Sleep Medicine, Department of Medicine, University of California San Francisco, San Francisco, California, USA
| | - Yong Zhou
- Division of Pulmonary, Allergy and Critical Care Medicine, Department of Medicine, University of Alabama at Birmingham, Alabama, USA
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8
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Jaumouillé V. Measurement of Minute Cellular Forces by Traction Force Microscopy. Methods Mol Biol 2022; 2440:125-139. [PMID: 35218537 DOI: 10.1007/978-1-0716-2051-9_8] [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] [Indexed: 06/14/2023]
Abstract
The ability of living cells to exert forces on their surrounding environment, such as the extracellular matrix (ECM) or neighboring cells, plays an important role in numerous biological processes. This chapter describes a simple protocol to measure forces exerted by living cells using traction force microscopy. This approach is based on the measurement of the deformation of compliant substrates using fluorescent fiducials. It can be implemented using widefield or confocal fluorescent microscopes, and open-source software. This chapter describes a step-by-step protocol to measure forces exerted by focal adhesions bound to the ECM protein fibronectin. However, this framework is versatile and can be easily adapted to a multitude of ligands and cellular processes in which cells exert forces, including the formation of an immunological synapse or a phagocytic cup. Technical considerations, limitations of the approach, and practical advice are discussed.
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Affiliation(s)
- Valentin Jaumouillé
- Department of Molecular biology and Biochemistry, Simon Fraser University, Burnaby, BC, Canada.
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9
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Ghabache E, Cao Y, Miao Y, Groisman A, Devreotes PN, Rappel W. Coupling traction force patterns and actomyosin wave dynamics reveals mechanics of cell motion. Mol Syst Biol 2021; 17:e10505. [PMID: 34898015 PMCID: PMC8666840 DOI: 10.15252/msb.202110505] [Citation(s) in RCA: 2] [Impact Index Per Article: 0.7] [Reference Citation Analysis] [Abstract] [Key Words] [MESH Headings] [Grants] [Track Full Text] [Download PDF] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Received: 06/16/2021] [Revised: 11/18/2021] [Accepted: 11/19/2021] [Indexed: 11/13/2022] Open
Abstract
Motile cells can use and switch between different modes of migration. Here, we use traction force microscopy and fluorescent labeling of actin and myosin to quantify and correlate traction force patterns and cytoskeletal distributions in Dictyostelium discoideum cells that move and switch between keratocyte-like fan-shaped, oscillatory, and amoeboid modes. We find that the wave dynamics of the cytoskeletal components critically determine the traction force pattern, cell morphology, and migration mode. Furthermore, we find that fan-shaped cells can exhibit two different propulsion mechanisms, each with a distinct traction force pattern. Finally, the traction force patterns can be recapitulated using a computational model, which uses the experimentally determined spatiotemporal distributions of actin and myosin forces and a viscous cytoskeletal network. Our results suggest that cell motion can be generated by friction between the flow of this network and the substrate.
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Affiliation(s)
| | - Yuansheng Cao
- Department of PhysicsUniversity of California, San DiegoLa JollaCAUSA
| | - Yuchuan Miao
- Department of Cell BiologySchool of MedicineJohns Hopkins UniversityBaltimoreMDUSA
| | - Alex Groisman
- Department of PhysicsUniversity of California, San DiegoLa JollaCAUSA
| | - Peter N Devreotes
- Department of Cell BiologySchool of MedicineJohns Hopkins UniversityBaltimoreMDUSA
| | - Wouter‐Jan Rappel
- Department of PhysicsUniversity of California, San DiegoLa JollaCAUSA
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10
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Hobson CM, Aaron JS, Heddleston JM, Chew TL. Visualizing the Invisible: Advanced Optical Microscopy as a Tool to Measure Biomechanical Forces. Front Cell Dev Biol 2021; 9:706126. [PMID: 34552926 PMCID: PMC8450411 DOI: 10.3389/fcell.2021.706126] [Citation(s) in RCA: 4] [Impact Index Per Article: 1.3] [Reference Citation Analysis] [Abstract] [Key Words] [Track Full Text] [Download PDF] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Received: 05/06/2021] [Accepted: 08/09/2021] [Indexed: 01/28/2023] Open
Abstract
The importance of mechanical force in biology is evident across diverse length scales, ranging from tissue morphogenesis during embryo development to mechanotransduction across single adhesion proteins at the cell surface. Consequently, many force measurement techniques rely on optical microscopy to measure forces being applied by cells on their environment, to visualize specimen deformations due to external forces, or even to directly apply a physical perturbation to the sample via photoablation or optogenetic tools. Recent developments in advanced microscopy offer improved approaches to enhance spatiotemporal resolution, imaging depth, and sample viability. These advances can be coupled with already existing force measurement methods to improve sensitivity, duration and speed, amongst other parameters. However, gaining access to advanced microscopy instrumentation and the expertise necessary to extract meaningful insights from these techniques is an unavoidable hurdle. In this Live Cell Imaging special issue Review, we survey common microscopy-based force measurement techniques and examine how they can be bolstered by emerging microscopy methods. We further explore challenges related to the accompanying data analysis in biomechanical studies and discuss the various resources available to tackle the global issue of technology dissemination, an important avenue for biologists to gain access to pre-commercial instruments that can be leveraged for biomechanical studies.
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Affiliation(s)
- Chad M. Hobson
- Advanced Imaging Center, Janelia Research Campus, Howard Hughes Medical Institute, Ashburn, VA, United States
| | - Jesse S. Aaron
- Advanced Imaging Center, Janelia Research Campus, Howard Hughes Medical Institute, Ashburn, VA, United States
| | - John M. Heddleston
- Cleveland Clinic Florida Research and Innovation Center, Port St. Lucie, FL, United States
| | - Teng-Leong Chew
- Advanced Imaging Center, Janelia Research Campus, Howard Hughes Medical Institute, Ashburn, VA, United States
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11
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Korobchevskaya K, Colin-York H, Barbieri L, Fritzsche M. Extended mechanical force measurements using structured illumination microscopy. PHILOSOPHICAL TRANSACTIONS. SERIES A, MATHEMATICAL, PHYSICAL, AND ENGINEERING SCIENCES 2021; 379:20200151. [PMID: 33896200 PMCID: PMC7612033 DOI: 10.1098/rsta.2020.0151] [Citation(s) in RCA: 0] [Impact Index Per Article: 0] [Reference Citation Analysis] [Abstract] [Key Words] [MESH Headings] [Grants] [Track Full Text] [Subscribe] [Scholar Register] [Accepted: 01/11/2021] [Indexed: 06/12/2023]
Abstract
Quantifying cell generated mechanical forces is key to furthering our understanding of mechanobiology. Traction force microscopy (TFM) is one of the most broadly applied force probing technologies, but its sensitivity is strictly dependent on the spatio-temporal resolution of the underlying imaging system. In previous works, it was demonstrated that increased sampling densities of cell derived forces permitted by super-resolution fluorescence imaging enhanced the sensitivity of the TFM method. However, these recent advances to TFM based on super-resolution techniques were limited to slow acquisition speeds and high illumination powers. Here, we present three novel TFM approaches that, in combination with total internal reflection, structured illumination microscopy and astigmatism, improve the spatial and temporal performance in either two-dimensional or three-dimensional mechanical force quantification, while maintaining low illumination powers. These three techniques can be straightforwardly implemented on a single optical set-up offering a powerful platform to provide new insights into the physiological force generation in a wide range of biological studies. This article is part of the Theo Murphy meeting issue 'Super-resolution structured illumination microscopy (part 1)'.
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Affiliation(s)
- Kseniya Korobchevskaya
- Kennedy Institute for Rheumatology, Roosevelt Drive, University of Oxford, Oxford, OX3 7LF, United Kingdom
| | - Huw Colin-York
- Kennedy Institute for Rheumatology, Roosevelt Drive, University of Oxford, Oxford, OX3 7LF, United Kingdom
| | - Liliana Barbieri
- MRC Human Immunology Unit, Weatherall Institute of Molecular Medicine, University of Oxford, Headley Way, Oxford. OX3 9DS, United Kingdom
| | - Marco Fritzsche
- Kennedy Institute for Rheumatology, Roosevelt Drive, University of Oxford, Oxford, OX3 7LF, United Kingdom
- MRC Human Immunology Unit, Weatherall Institute of Molecular Medicine, University of Oxford, Headley Way, Oxford. OX3 9DS, United Kingdom
- Rosalind Franklin Institute, Harwell Campus, Didcot, OX11 0FA, United Kingdom
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12
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Barbieri L, Colin-York H, Korobchevskaya K, Li D, Wolfson DL, Karedla N, Schneider F, Ahluwalia BS, Seternes T, Dalmo RA, Dustin ML, Li D, Fritzsche M. Two-dimensional TIRF-SIM-traction force microscopy (2D TIRF-SIM-TFM). Nat Commun 2021; 12:2169. [PMID: 33846317 PMCID: PMC8041833 DOI: 10.1038/s41467-021-22377-9] [Citation(s) in RCA: 22] [Impact Index Per Article: 7.3] [Reference Citation Analysis] [Abstract] [Key Words] [MESH Headings] [Grants] [Track Full Text] [Download PDF] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Received: 06/01/2020] [Accepted: 03/12/2021] [Indexed: 02/01/2023] Open
Abstract
Quantifying small, rapidly evolving forces generated by cells is a major challenge for the understanding of biomechanics and mechanobiology in health and disease. Traction force microscopy remains one of the most broadly applied force probing technologies but typically restricts itself to slow events over seconds and micron-scale displacements. Here, we improve >2-fold spatially and >10-fold temporally the resolution of planar cellular force probing compared to its related conventional modalities by combining fast two-dimensional total internal reflection fluorescence super-resolution structured illumination microscopy and traction force microscopy. This live-cell 2D TIRF-SIM-TFM methodology offers a combination of spatio-temporal resolution enhancement relevant to forces on the nano- and sub-second scales, opening up new aspects of mechanobiology to analysis.
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Grants
- Biotechnology and Biological Sciences Research Council
- 212343/Z/18/Z Wellcome Trust
- 107457 Wellcome Trust
- 100262/Z/12/Z Wellcome Trust
- Wellcome Trust
- 091911 Wellcome Trust
- Medical Research Council
- L.B. would like to acknowledge funding from the Engineering and Physical Sciences Research Council (EPSRC) and Medical Research Council (EP/L016052/1). M.F., H.C.Y., K.K., and M.L.D. would like to thank the Rosalind Franklin Institute and the Kennedy Trust for Rheumatology Research (KTRR) for support. M.F., F.S., and H.C.Y. thank the Wellcome Trust (212343/Z/18/Z) and EPSRC (EP/S004459/1). M.L.D. also thank the Wellcome Trust for the Principal Research Fellowship awarded to M.D. (100262/Z/12/Z). Di.L. and D.L. are supported by a grant from the Chinese Ministry of Science and Technology (MOST: 2017YFA0505301, 2016YFA0500203), the National Natural Science Foundation of China (NSFC; 91754202, 31827802), and the Youth Innovation Promotion Association of Chinese Academy of Sciences (Grant No. 2020094). N.K. thanks the Alexander von Humboldt Foundation for funding his Feoder Lynen Fellowship. R.A.D acknowledge the Research Council of Norway (grant no. 301401) for funding. The TIRF-SIM platform was built in collaboration with and with funds from Micron (www.micronoxford.com), an Oxford-wide advanced microscopy technology consortium supported by Wellcome Strategic Awards (091911 and 107457) and an MRC/EPSRC/BBSRC next generation imaging award.
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Affiliation(s)
- Liliana Barbieri
- MRC Human Immunology Unit, Weatherall Institute of Molecular Medicine, University of Oxford, Oxford, UK
| | - Huw Colin-York
- MRC Human Immunology Unit, Weatherall Institute of Molecular Medicine, University of Oxford, Oxford, UK
- Kennedy Institute for Rheumatology, University of Oxford, Oxford, UK
| | | | - Di Li
- National Laboratory of Biomacromolecules, Institute of Biophysics, Chinese Academy of Sciences, Beijing, China
| | - Deanna L Wolfson
- Department of Physics and Technology, UiT The Arctic University of Norway, Tromsø, Norway
| | - Narain Karedla
- Kennedy Institute for Rheumatology, University of Oxford, Oxford, UK
- Rosalind Franklin Institute, Didcot, UK
| | - Falk Schneider
- MRC Human Immunology Unit, Weatherall Institute of Molecular Medicine, University of Oxford, Oxford, UK
- Kennedy Institute for Rheumatology, University of Oxford, Oxford, UK
| | - Balpreet S Ahluwalia
- Department of Physics and Technology, UiT The Arctic University of Norway, Tromsø, Norway
| | - Tore Seternes
- Norwegian College of Fishery Science, UiT The Arctic University of Norway, Tromsø, Norway
| | - Roy A Dalmo
- Norwegian College of Fishery Science, UiT The Arctic University of Norway, Tromsø, Norway
| | - Michael L Dustin
- Kennedy Institute for Rheumatology, University of Oxford, Oxford, UK
| | - Dong Li
- National Laboratory of Biomacromolecules, Institute of Biophysics, Chinese Academy of Sciences, Beijing, China.
- College of Life Sciences, University of Chinese Academy of Sciences, Beijing, China.
| | - Marco Fritzsche
- MRC Human Immunology Unit, Weatherall Institute of Molecular Medicine, University of Oxford, Oxford, UK.
- Kennedy Institute for Rheumatology, University of Oxford, Oxford, UK.
- Rosalind Franklin Institute, Didcot, UK.
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13
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Li D, Colin-York H, Barbieri L, Javanmardi Y, Guo Y, Korobchevskaya K, Moeendarbary E, Li D, Fritzsche M. Astigmatic traction force microscopy (aTFM). Nat Commun 2021; 12:2168. [PMID: 33846322 PMCID: PMC8042066 DOI: 10.1038/s41467-021-22376-w] [Citation(s) in RCA: 26] [Impact Index Per Article: 8.7] [Reference Citation Analysis] [Abstract] [Key Words] [MESH Headings] [Grants] [Track Full Text] [Download PDF] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Received: 06/01/2020] [Accepted: 03/12/2021] [Indexed: 01/23/2023] Open
Abstract
Quantifying small, rapidly progressing three-dimensional forces generated by cells remains a major challenge towards a more complete understanding of mechanobiology. Traction force microscopy is one of the most broadly applied force probing technologies but ascertaining three-dimensional information typically necessitates slow, multi-frame z-stack acquisition with limited sensitivity. Here, by performing traction force microscopy using fast single-frame astigmatic imaging coupled with total internal reflection fluorescence microscopy we improve the temporal resolution of three-dimensional mechanical force quantification up to 10-fold compared to its related super-resolution modalities. 2.5D astigmatic traction force microscopy (aTFM) thus enables live-cell force measurements approaching physiological sensitivity.
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Affiliation(s)
- Di Li
- National Laboratory of Biomacromolecules, CAS Center for Excellence in Biomacromolecules, Institute of Biophysics, Chinese Academy of Sciences, Beijing, China
| | - Huw Colin-York
- MRC Human Immunology Unit, Weatherall Institute of Molecular Medicine, University of Oxford, Oxford, UK
- Kennedy Institute for Rheumatology, University of Oxford, Oxford, UK
| | - Liliana Barbieri
- MRC Human Immunology Unit, Weatherall Institute of Molecular Medicine, University of Oxford, Oxford, UK
| | - Yousef Javanmardi
- Department of Mechanical Engineering, University College London, London, UK
| | - Yuting Guo
- National Laboratory of Biomacromolecules, CAS Center for Excellence in Biomacromolecules, Institute of Biophysics, Chinese Academy of Sciences, Beijing, China
| | | | - Emad Moeendarbary
- Department of Mechanical Engineering, University College London, London, UK.
| | - Dong Li
- National Laboratory of Biomacromolecules, CAS Center for Excellence in Biomacromolecules, Institute of Biophysics, Chinese Academy of Sciences, Beijing, China.
- College of Life Sciences, University of Chinese Academy of Sciences, Beijing, China.
| | - Marco Fritzsche
- MRC Human Immunology Unit, Weatherall Institute of Molecular Medicine, University of Oxford, Oxford, UK.
- Kennedy Institute for Rheumatology, University of Oxford, Oxford, UK.
- Rosalind Franklin Institute, Harwell Campus, Didcot, UK.
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14
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Han SJ, Azarova EV, Whitewood AJ, Bachir A, Guttierrez E, Groisman A, Horwitz AR, Goult BT, Dean KM, Danuser G. Pre-complexation of talin and vinculin without tension is required for efficient nascent adhesion maturation. eLife 2021; 10:66151. [PMID: 33783351 PMCID: PMC8009661 DOI: 10.7554/elife.66151] [Citation(s) in RCA: 28] [Impact Index Per Article: 9.3] [Reference Citation Analysis] [Abstract] [Key Words] [Track Full Text] [Download PDF] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Received: 12/30/2020] [Accepted: 03/11/2021] [Indexed: 12/23/2022] Open
Abstract
Talin and vinculin are mechanosensitive proteins that are recruited early to integrin-based nascent adhesions (NAs). In two epithelial cell systems with well-delineated NA formation, we find these molecules concurrently recruited to the subclass of NAs maturing to focal adhesions. After the initial recruitment under minimal load, vinculin accumulates in maturing NAs at a ~ fivefold higher rate than in non-maturing NAs, and is accompanied by a faster traction force increase. We identify the R8 domain in talin, which exposes a vinculin-binding-site (VBS) in the absence of load, as required for NA maturation. Disruption of R8 domain function reduces load-free vinculin binding to talin, and reduces the rate of additional vinculin recruitment. Taken together, these data show that the concurrent recruitment of talin and vinculin prior to mechanical engagement with integrins is essential for the traction-mediated unfolding of talin, exposure of additional VBSs, further recruitment of vinculin, and ultimately, NA maturation.
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Affiliation(s)
- Sangyoon J Han
- Lyda Hill Department of Bioinformatics, University of Texas Southwestern Medical Center, Dallas, United States.,Department of Biomedical Engineering, Michigan Technological University, Houghton, United States
| | - Evgenia V Azarova
- Department of Cell Biology, University of Texas Southwestern Medical Center, Dallas, United States
| | | | - Alexia Bachir
- Department of Cell Biology, University of Virginia, Charlottesville, United States
| | - Edgar Guttierrez
- Department of Physics, University of California San Diego, San Diego, United States
| | - Alex Groisman
- Department of Physics, University of California San Diego, San Diego, United States
| | - Alan R Horwitz
- Department of Cell Biology, University of Virginia, Charlottesville, United States
| | - Benjamin T Goult
- School of Biosciences, University of Kent, Canterbury, United Kingdom
| | - Kevin M Dean
- Department of Cell Biology, University of Texas Southwestern Medical Center, Dallas, United States
| | - Gaudenz Danuser
- Lyda Hill Department of Bioinformatics, University of Texas Southwestern Medical Center, Dallas, United States.,Department of Cell Biology, University of Texas Southwestern Medical Center, Dallas, United States
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15
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Aramesh M, Mergenthal S, Issler M, Plochberger B, Weber F, Qin XH, Liska R, Duda GN, Huppa JB, Ries J, Schütz GJ, Klotzsch E. Functionalized Bead Assay to Measure Three-dimensional Traction Forces during T-cell Activation. NANO LETTERS 2021; 21:507-514. [PMID: 33305952 DOI: 10.1021/acs.nanolett.0c03964] [Citation(s) in RCA: 27] [Impact Index Per Article: 9.0] [Reference Citation Analysis] [Abstract] [Key Words] [MESH Headings] [Track Full Text] [Subscribe] [Scholar Register] [Indexed: 06/12/2023]
Abstract
When T-cells probe their environment for antigens, the bond between the T-cell receptor (TCR) and the peptide-loaded major histocompatibility complex (MHC) is put under tension, thereby influencing the antigen discrimination. Yet, the quantification of such forces in the context of T-cell signaling is technically challenging. Here, we developed a traction force microscopy platform which allows for quantifying the pulls and pushes exerted via T-cell microvilli, in both tangential and normal directions, during T-cell activation. We immobilized specific T-cell activating antibodies on the marker beads used to read out the hydrogel deformation. Microvilli targeted the functionalized beads, as confirmed by superresolution microscopy of the local actin organization. Moreover, we found that cellular components, such as actin, TCR, and CD45 reorganize upon interaction with the beads, such that actin forms a vortex-like ring structure around the beads and TCR is enriched at the bead surface, whereas CD45 is excluded from bead-microvilli contacts.
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Affiliation(s)
- Morteza Aramesh
- Laboratory of Applied Mechanobiology, Department for Health Sciences and Technology, ETH Zürich, 8093 Zürich, Switzerland
| | - Simon Mergenthal
- Institute of Biology, Experimental Biophysics/Mechanobiology, Humboldt Universität zu Berlin, 10115 Berlin, Germany
| | - Marcel Issler
- Institute of Biology, Experimental Biophysics/Mechanobiology, Humboldt Universität zu Berlin, 10115 Berlin, Germany
| | - Birgit Plochberger
- Upper Austria University of Applied Sciences, Campus Linz, Garnisonstrasse 21, 4020 Linz, Austria
| | - Florian Weber
- Upper Austria University of Applied Sciences, Campus Linz, Garnisonstrasse 21, 4020 Linz, Austria
| | - Xiao-Hua Qin
- Institute for Biomechanics, Department for Health Sciences and Technology, ETH Zürich, 8093 Zürich, Switzerland
| | - Robert Liska
- Institute of Applied Synthetic Chemistry, TU Wien, Getreidemarkt 9/163/MC, 1060 Vienna, Austria
| | - Georg N Duda
- Julius Wolff Institute for Biomechanics and Musculoskeletal Regeneration, Charité-Universitätsmedizin, BIH Center for Regenerative Therapies, Berlin Institute of Health, 13353 Berlin, Germany
| | - Johannes B Huppa
- Institute for Hygiene and Applied Immunology, Center for Pathophysiology, Infectiology and Immunology, Medical University of Vienna, 1090 Vienna, Austria
| | - Jonas Ries
- EMBL Heidelberg, Meyerhofstraße 1, 69117 Heidelberg, Germany
| | | | - Enrico Klotzsch
- Laboratory of Applied Mechanobiology, Department for Health Sciences and Technology, ETH Zürich, 8093 Zürich, Switzerland
- Institute of Biology, Experimental Biophysics/Mechanobiology, Humboldt Universität zu Berlin, 10115 Berlin, Germany
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16
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Missirlis D, Haraszti T, Heckmann L, Spatz JP. Substrate Resistance to Traction Forces Controls Fibroblast Polarization. Biophys J 2020; 119:2558-2572. [PMID: 33217384 DOI: 10.1016/j.bpj.2020.10.043] [Citation(s) in RCA: 6] [Impact Index Per Article: 1.5] [Reference Citation Analysis] [Abstract] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Received: 05/15/2020] [Revised: 10/21/2020] [Accepted: 10/23/2020] [Indexed: 12/25/2022] Open
Abstract
The mechanics of fibronectin-rich extracellular matrix regulate cell physiology in a number of diseases, prompting efforts to elucidate cell mechanosensing mechanisms at the molecular and cellular scale. Here, the use of fibronectin-functionalized silicone elastomers that exhibit considerable frequency dependence in viscoelastic properties unveiled the presence of two cellular processes that respond discreetly to substrate mechanical properties. Weakly cross-linked elastomers supported efficient focal adhesion maturation and fibroblast spreading because of an apparent stiff surface layer. However, they did not enable cytoskeletal and fibroblast polarization; elastomers with high cross-linking and low deformability were required for polarization. Our results suggest as an underlying reason for this behavior the inability of soft elastomer substrates to resist traction forces rather than a lack of sufficient traction force generation. Accordingly, mild inhibition of actomyosin contractility rescued fibroblast polarization even on the softer elastomers. Our findings demonstrate differential dependence of substrate physical properties on distinct mechanosensitive processes and provide a premise to reconcile previously proposed local and global models of cell mechanosensing.
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Affiliation(s)
- Dimitris Missirlis
- Max-Planck-Institute for Medical Research, Department of Cellular Biophysics, Heidelberg, Germany.
| | - Tamás Haraszti
- DWI-Leibniz Institute for Interactive Materials, Aachen, Germany; RWTH Aachen University, Institute for Technical and Macromolecular Chemistry, Aachen, Germany
| | - Lara Heckmann
- Max-Planck-Institute for Medical Research, Department of Cellular Biophysics, Heidelberg, Germany
| | - Joachim P Spatz
- Max-Planck-Institute for Medical Research, Department of Cellular Biophysics, Heidelberg, Germany; Heidelberg University, Department of Biophysical Chemistry, Physical Chemistry Institute, Heidelberg, Germany
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17
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Dawson MR, Xuan B, Hsu J, Ghosh D. Force balancing ACT-IN the tumor microenvironment: Cytoskeletal modifications in cancer and stromal cells to promote malignancy. INTERNATIONAL REVIEW OF CELL AND MOLECULAR BIOLOGY 2020; 360:1-31. [PMID: 33962748 DOI: 10.1016/bs.ircmb.2020.09.005] [Citation(s) in RCA: 2] [Impact Index Per Article: 0.5] [Reference Citation Analysis] [Abstract] [Key Words] [Track Full Text] [Subscribe] [Scholar Register] [Indexed: 02/06/2023]
Abstract
The tumor microenvironment is a complex milieu that dictates the growth, invasion, and metastasis of cancer cells. Both cancer and stromal cells in the tumor tissue encounter and adapt to a variety of extracellular factors, and subsequently contribute and drive the progression of the disease to more advanced stages. As the disease progresses, a small population of cancer cells becomes more invasive through a complex process known as epithelial-mesenchymal transition, and nearby stromal cells assume a carcinoma associated fibroblast phenotype characterized by enhanced migration, cell contractility, and matrix secretion with the ability to reorganize extracellular matrices. As cells transition into more malignant phenotypes their biophysical properties, controlled by the organization of cytoskeletal proteins, are altered. Actin and its associated proteins are essential modulators and facilitators of these changes. As the cells respond to the cues in the microenvironment, actin driven mechanical forces inside and outside the cells also evolve. Recent advances in biophysical techniques have enabled us to probe these actin driven changes in cancer and stromal cells and demarcate their role in driving changes in the microenvironment. Understanding the underlying biophysical mechanisms that drive cancer progression could provide critical insight on novel therapeutic approaches in the fight against cancer.
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Affiliation(s)
- Michelle R Dawson
- Department of Molecular Pharmacology, Physiology, and Biotechnology, Brown University, Providence, RI, United States; Department of Molecular Biology, Cell Biology and Biochemistry, Brown University, Providence, RI, United States; Brown University, Center for Biomedical Engineering, Providence, RI, United States.
| | - Botai Xuan
- Department of Molecular Pharmacology, Physiology, and Biotechnology, Brown University, Providence, RI, United States
| | - Jeffrey Hsu
- Department of Molecular Pharmacology, Physiology, and Biotechnology, Brown University, Providence, RI, United States
| | - Deepraj Ghosh
- Department of Molecular Pharmacology, Physiology, and Biotechnology, Brown University, Providence, RI, United States
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18
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Allen GM, Lee KC, Barnhart EL, Tsuchida MA, Wilson CA, Gutierrez E, Groisman A, Theriot JA, Mogilner A. Cell Mechanics at the Rear Act to Steer the Direction of Cell Migration. Cell Syst 2020; 11:286-299.e4. [PMID: 32916096 PMCID: PMC7530145 DOI: 10.1016/j.cels.2020.08.008] [Citation(s) in RCA: 9] [Impact Index Per Article: 2.3] [Reference Citation Analysis] [Abstract] [Key Words] [MESH Headings] [Grants] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Received: 04/22/2020] [Revised: 06/17/2020] [Accepted: 08/10/2020] [Indexed: 01/18/2023]
Abstract
Motile cells navigate complex environments by changing their direction of travel, generating left-right asymmetries in their mechanical subsystems to physically turn. Currently, little is known about how external directional cues are propagated along the length scale of the whole cell and integrated with its force-generating apparatus to steer migration mechanically. We examine the mechanics of spontaneous cell turning in fish epidermal keratocytes and find that the mechanical asymmetries responsible for turning behavior predominate at the rear of the cell, where there is asymmetric centripetal actin flow. Using experimental perturbations, we identify two linked feedback loops connecting myosin II contractility, adhesion strength and actin network flow in turning cells that are sufficient to explain the observed cell shapes and trajectories. Notably, asymmetries in actin polymerization at the cell leading edge play only a minor role in the mechanics of cell turning-that is, cells steer from the rear.
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Affiliation(s)
- Greg M Allen
- Department of Biochemistry and Howard Hughes Medical Institute, Stanford University School of Medicine, Stanford, CA 94305, USA
| | - Kun Chun Lee
- Department of Neurobiology, Physiology and Behavior, University of California, Davis, Davis, CA 95616, USA
| | - Erin L Barnhart
- Department of Biochemistry and Howard Hughes Medical Institute, Stanford University School of Medicine, Stanford, CA 94305, USA
| | - Mark A Tsuchida
- Department of Biochemistry and Howard Hughes Medical Institute, Stanford University School of Medicine, Stanford, CA 94305, USA
| | - Cyrus A Wilson
- Department of Biochemistry and Howard Hughes Medical Institute, Stanford University School of Medicine, Stanford, CA 94305, USA
| | - Edgar Gutierrez
- Department of Physics, University of California, San Diego, San Diego, CA 92023, USA
| | - Alexander Groisman
- Department of Physics, University of California, San Diego, San Diego, CA 92023, USA
| | - Julie A Theriot
- Department of Biology and Howard Hughes Medical Institute, University of Washington, Seattle, WA 98195, USA.
| | - Alex Mogilner
- Courant Institute of Mathematical Sciences and Department of Biology, New York University, New York, NY 10012, USA.
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19
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Rochman ND, Yao K, Gonzalez NPA, Wirtz D, Sun SX. Single Cell Volume Measurement Utilizing the Fluorescence Exclusion Method (FXm). Bio Protoc 2020; 10:e3652. [PMID: 33659322 DOI: 10.21769/bioprotoc.3652] [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: 12/23/2019] [Revised: 04/13/2020] [Accepted: 04/28/2020] [Indexed: 01/28/2023] Open
Abstract
The measurement of single cell size remains an obstacle towards a deeper understanding of cell growth control, tissue homeostasis, organogenesis, and a wide range of pathologies. Recent advances have placed a spotlight on the importance of cell volume in the regulation of fundamental cell signaling pathways including those known to orchestrate progression through the cell cycle. Here we provide our protocol for the Fluorescence Exclusion Method (FXm); references to the development of FXm; and a brief outlook on future advances in image analysis which may expand the range of problems studied utilizing FXm as well as lower the barrier to entry for groups interested in adding cell volume measurements into their experimental repertoire.
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Affiliation(s)
- Nash D Rochman
- Department of Chemical and Biomolecular Engineering, Johns Hopkins University, Baltimore, Maryland 21218, USA
| | - Kai Yao
- Department of Mechanical Engineering, Johns Hopkins University, Baltimore, Maryland 21218, USA
| | - Nicolas Perez A Gonzalez
- Department of Chemical and Biomolecular Engineering, Johns Hopkins University, Baltimore, Maryland 21218, USA
| | - Denis Wirtz
- Department of Chemical and Biomolecular Engineering, Johns Hopkins University, Baltimore, Maryland 21218, USA.,Physical Sciences in Oncology Center (PSOC), Johns Hopkins University, Baltimore, Maryland 21218, USA
| | - Sean X Sun
- Department of Chemical and Biomolecular Engineering, Johns Hopkins University, Baltimore, Maryland 21218, USA.,Department of Mechanical Engineering, Johns Hopkins University, Baltimore, Maryland 21218, USA.,Physical Sciences in Oncology Center (PSOC), Johns Hopkins University, Baltimore, Maryland 21218, USA
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20
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Prusakov KA, Bagrov DV, Basmanov DV, Romanov SA, Klinov DV. Fluorescence imaging of cells using long-range electromagnetic surface waves for excitation. APPLIED OPTICS 2020; 59:4833-4838. [PMID: 32543477 DOI: 10.1364/ao.389120] [Citation(s) in RCA: 1] [Impact Index Per Article: 0.3] [Reference Citation Analysis] [Abstract] [MESH Headings] [Track Full Text] [Subscribe] [Scholar Register] [Received: 01/24/2020] [Accepted: 04/22/2020] [Indexed: 06/11/2023]
Abstract
We present a depth-localized illumination technique for wide-field fluorescence microscopy, based on long-range optical surface waves. This technique allows one to excite the fluorescence only in a thin near-substrate layer of the specimen. Our experimental setup is compatible with both upright and inverted microscopes. It provides fluorescent microscopic images, which are superior to the epifluorescence ones in signal-to-noise ratio, contrast, and detail. We demonstrate the applicability of our technique for imaging both bacterial and eukaryotic cells (E. coli and HeLa, respectively).
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21
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Stubb A, Laine RF, Miihkinen M, Hamidi H, Guzmán C, Henriques R, Jacquemet G, Ivaska J. Fluctuation-Based Super-Resolution Traction Force Microscopy. NANO LETTERS 2020; 20:2230-2245. [PMID: 32142297 PMCID: PMC7146861 DOI: 10.1021/acs.nanolett.9b04083] [Citation(s) in RCA: 36] [Impact Index Per Article: 9.0] [Reference Citation Analysis] [Abstract] [Key Words] [MESH Headings] [Grants] [Track Full Text] [Subscribe] [Scholar Register] [Received: 10/03/2019] [Revised: 03/02/2020] [Indexed: 05/24/2023]
Abstract
Cellular mechanics play a crucial role in tissue homeostasis and are often misregulated in disease. Traction force microscopy is one of the key methods that has enabled researchers to study fundamental aspects of mechanobiology; however, traction force microscopy is limited by poor resolution. Here, we propose a simplified protocol and imaging strategy that enhances the output of traction force microscopy by increasing i) achievable bead density and ii) the accuracy of bead tracking. Our approach relies on super-resolution microscopy, enabled by fluorescence fluctuation analysis. Our pipeline can be used on spinning-disk confocal or widefield microscopes and is compatible with available analysis software. In addition, we demonstrate that our workflow can be used to gain biologically relevant information and is suitable for fast long-term live measurement of traction forces even in light-sensitive cells. Finally, using fluctuation-based traction force microscopy, we observe that filopodia align to the force field generated by focal adhesions.
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Affiliation(s)
- Aki Stubb
- Turku
Bioscience Centre, University of Turku and
Åbo Akademi University, FI-20520 Turku, Finland
| | - Romain F. Laine
- MRC-Laboratory
for Molecular Cell Biology, University College
London, London WC1E 6BT, U.K.
- The
Francis Crick Institute, London NW1 1AT, U.K.
| | - Mitro Miihkinen
- Turku
Bioscience Centre, University of Turku and
Åbo Akademi University, FI-20520 Turku, Finland
| | - Hellyeh Hamidi
- Turku
Bioscience Centre, University of Turku and
Åbo Akademi University, FI-20520 Turku, Finland
| | - Camilo Guzmán
- Turku
Bioscience Centre, University of Turku and
Åbo Akademi University, FI-20520 Turku, Finland
| | - Ricardo Henriques
- MRC-Laboratory
for Molecular Cell Biology, University College
London, London WC1E 6BT, U.K.
- The
Francis Crick Institute, London NW1 1AT, U.K.
| | - Guillaume Jacquemet
- Turku
Bioscience Centre, University of Turku and
Åbo Akademi University, FI-20520 Turku, Finland
- Faculty
of Science and Engineering, Cell Biology, Åbo Akademi University, 20520 Turku, Finland
| | - Johanna Ivaska
- Turku
Bioscience Centre, University of Turku and
Åbo Akademi University, FI-20520 Turku, Finland
- Department
of Biochemistry, University of Turku, FIN-20520 Turku, Finland
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22
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Cheng Z, Shurer CR, Schmidt S, Gupta VK, Chuang G, Su J, Watkins AR, Shetty A, Spector JA, Hui CY, Reesink HL, Paszek MJ. The surface stress of biomedical silicones is a stimulant of cellular response. SCIENCE ADVANCES 2020; 6:eaay0076. [PMID: 32300645 PMCID: PMC7148089 DOI: 10.1126/sciadv.aay0076] [Citation(s) in RCA: 15] [Impact Index Per Article: 3.8] [Reference Citation Analysis] [Abstract] [MESH Headings] [Grants] [Track Full Text] [Download PDF] [Figures] [Subscribe] [Scholar Register] [Received: 05/15/2019] [Accepted: 01/08/2020] [Indexed: 06/11/2023]
Abstract
Silicones are commonly used for lubrication of syringes, encapsulation of medical devices, and fabrication of surgical implants. While silicones are generally viewed as relatively inert to the cellular milieu, they can mediate a variety of inflammatory responses and other deleterious effects, but the mechanisms underlying the bioactivity of silicones remain unresolved. Here, we report that silicone liquids and gels have high surface stresses that can strongly resist deformation at cellular length scales. Biomedical silicones, including syringe lubricants and fillings from FDA-approved breast implants, readily adsorb matrix proteins and activate canonical rigidity sensing pathways through their surface stresses. In 3D culture models, liquid silicone droplets support robust cellular adhesion and the formation of multinucleated monocyte-derived cell masses that recapitulate phenotypic aspects of granuloma formation in the foreign body response. Together, our findings implicate surface stress as a cellular stimulant that should be considered in application of silicones for biomedical purposes.
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Affiliation(s)
- Zhu Cheng
- Robert Frederick Smith School of Chemical and Biomolecular Engineering, Cornell University, Ithaca, NY 14853, USA
| | - Carolyn R. Shurer
- Robert Frederick Smith School of Chemical and Biomolecular Engineering, Cornell University, Ithaca, NY 14853, USA
| | - Samuel Schmidt
- Robert Frederick Smith School of Chemical and Biomolecular Engineering, Cornell University, Ithaca, NY 14853, USA
- Kavli Institute at Cornell for Nanoscale Science, Ithaca, NY 14853, USA
| | - Vivek K. Gupta
- Sibley School of Mechanical and Aerospace Engineering, Cornell University, Ithaca, NY 14853, USA
- Department of Mechanical Engineering, Stanford University, CA 94305, USA
| | - Grace Chuang
- Robert Frederick Smith School of Chemical and Biomolecular Engineering, Cornell University, Ithaca, NY 14853, USA
| | - Jin Su
- College of Veterinary Medicine, Cornell University, Ithaca, NY 14853, USA
| | - Amanda R. Watkins
- College of Veterinary Medicine, Cornell University, Ithaca, NY 14853, USA
| | - Abhishek Shetty
- Rheology Department, Anton Paar USA Inc., Ashland, VA 23005, USA
| | - Jason A. Spector
- Weill Cornell Medicine, Cornell University, New York, NY 10065, USA
| | - Chung-Yuen Hui
- Sibley School of Mechanical and Aerospace Engineering, Cornell University, Ithaca, NY 14853, USA
- Field of Theoretical and Applied Mechanics, Cornell University, Ithaca, NY 14853, USA
| | - Heidi L. Reesink
- College of Veterinary Medicine, Cornell University, Ithaca, NY 14853, USA
| | - Matthew J. Paszek
- Robert Frederick Smith School of Chemical and Biomolecular Engineering, Cornell University, Ithaca, NY 14853, USA
- Kavli Institute at Cornell for Nanoscale Science, Ithaca, NY 14853, USA
- Field of Biophysics, Cornell University, Ithaca, NY 14853, USA
- Field of Biomedical Engineering, Cornell University, Ithaca, NY 14853, USA
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23
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Force-dependent extracellular matrix remodeling by early-stage cancer cells alters diffusion and induces carcinoma-associated fibroblasts. Biomaterials 2020; 234:119756. [PMID: 31954229 DOI: 10.1016/j.biomaterials.2020.119756] [Citation(s) in RCA: 28] [Impact Index Per Article: 7.0] [Reference Citation Analysis] [Abstract] [Key Words] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Received: 09/19/2019] [Revised: 12/28/2019] [Accepted: 01/02/2020] [Indexed: 12/21/2022]
Abstract
It is known cancer cells secrete cytokines inducing normal fibroblasts (NFs) to become carcinoma-associated fibroblasts (CAFs). However, it is not clear how the CAF-promoting cytokines can effectively navigate the dense ECM, a diffusion barrier, in the tumor microenvironment to reach NFs during the early stages of cancer development. In this study, we devised a 3D coculture system to investigate the possible mechanism of CAF induction at early stages of breast cancer. We found that in a force-dependent manner, ECM fibrils are radially aligned relative to the tumor spheroid. The fibril alignment enhances the diffusion of exosomes containing CAF-promoting cytokines towards NFs. Suppression of force generation or ECM remodeling abolishes the enhancement of exosome diffusion and the subsequent CAF induction. In summary, our finding suggests that early-stage, pre-metastatic cancer cells can generate high forces to align the ECM fibrils, thereby enhancing the diffusion of CAF-promoting exosomes to reach the stroma and induce CAFs.
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24
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Mohan AS, Dean KM, Isogai T, Kasitinon SY, Murali VS, Roudot P, Groisman A, Reed DK, Welf ES, Han SJ, Noh J, Danuser G. Enhanced Dendritic Actin Network Formation in Extended Lamellipodia Drives Proliferation in Growth-Challenged Rac1 P29S Melanoma Cells. Dev Cell 2020; 49:444-460.e9. [PMID: 31063759 DOI: 10.1016/j.devcel.2019.04.007] [Citation(s) in RCA: 34] [Impact Index Per Article: 8.5] [Reference Citation Analysis] [Abstract] [Key Words] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Received: 08/15/2018] [Revised: 01/21/2019] [Accepted: 04/05/2019] [Indexed: 12/19/2022]
Abstract
Actin assembly supplies the structural framework for cell morphology and migration. Beyond structure, this actin framework can also be engaged to drive biochemical signaling programs. Here, we describe how the hyperactivation of Rac1 via the P29S mutation (Rac1P29S) in melanoma hijacks branched actin network assembly to coordinate proliferative cues that facilitate metastasis and drug resistance. Upon growth challenge, Rac1P29S-harboring melanoma cells massively upregulate lamellipodia formation by dendritic actin polymerization. These extended lamellipodia form a signaling microdomain that sequesters and phospho-inactivates the tumor suppressor NF2/Merlin, driving Rac1P29S cell proliferation in growth suppressive conditions. These biochemically active lamellipodia require cell-substrate attachment but not focal adhesion assembly and drive proliferation independently of the ERK/MAPK pathway. These data suggest a critical link between cell morphology and cell signaling and reconcile the dichotomy of Rac1's regulation of both proliferation and actin assembly by revealing a mutual signaling axis wherein actin assembly drives proliferation in melanoma.
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Affiliation(s)
- Ashwathi S Mohan
- Lyda Hill Department of Bioinformatics, University of Texas Southwestern Medical Center, Dallas, TX 75390, USA; Department of Cell Biology, University of Texas Southwestern Medical Center, Dallas, TX 75390, USA
| | - Kevin M Dean
- Department of Cell Biology, University of Texas Southwestern Medical Center, Dallas, TX 75390, USA
| | - Tadamoto Isogai
- Lyda Hill Department of Bioinformatics, University of Texas Southwestern Medical Center, Dallas, TX 75390, USA; Department of Cell Biology, University of Texas Southwestern Medical Center, Dallas, TX 75390, USA
| | - Stacy Y Kasitinon
- Children's Research Institute and the Department of Pediatrics, University of Texas Southwestern Medical Center, Dallas, TX 75390, USA
| | - Vasanth S Murali
- Lyda Hill Department of Bioinformatics, University of Texas Southwestern Medical Center, Dallas, TX 75390, USA
| | - Philippe Roudot
- Lyda Hill Department of Bioinformatics, University of Texas Southwestern Medical Center, Dallas, TX 75390, USA; Department of Cell Biology, University of Texas Southwestern Medical Center, Dallas, TX 75390, USA
| | - Alex Groisman
- Department of Physics, University of California, San Diego, La Jolla, CA 92093, USA
| | - Dana K Reed
- Lyda Hill Department of Bioinformatics, University of Texas Southwestern Medical Center, Dallas, TX 75390, USA; Department of Cell Biology, University of Texas Southwestern Medical Center, Dallas, TX 75390, USA
| | - Erik S Welf
- Lyda Hill Department of Bioinformatics, University of Texas Southwestern Medical Center, Dallas, TX 75390, USA; Department of Cell Biology, University of Texas Southwestern Medical Center, Dallas, TX 75390, USA
| | - Sangyoon J Han
- Lyda Hill Department of Bioinformatics, University of Texas Southwestern Medical Center, Dallas, TX 75390, USA; Department of Cell Biology, University of Texas Southwestern Medical Center, Dallas, TX 75390, USA; Department of Biomedical Engineering, Michigan Technological University, Houghton, MI 49931, USA
| | - Jungsik Noh
- Lyda Hill Department of Bioinformatics, University of Texas Southwestern Medical Center, Dallas, TX 75390, USA; Department of Cell Biology, University of Texas Southwestern Medical Center, Dallas, TX 75390, USA
| | - Gaudenz Danuser
- Lyda Hill Department of Bioinformatics, University of Texas Southwestern Medical Center, Dallas, TX 75390, USA; Department of Cell Biology, University of Texas Southwestern Medical Center, Dallas, TX 75390, USA.
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25
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Raghuwanshi VS, Garnier G. Characterisation of hydrogels: Linking the nano to the microscale. Adv Colloid Interface Sci 2019; 274:102044. [PMID: 31677493 DOI: 10.1016/j.cis.2019.102044] [Citation(s) in RCA: 54] [Impact Index Per Article: 10.8] [Reference Citation Analysis] [Abstract] [Key Words] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Received: 07/17/2019] [Revised: 09/26/2019] [Accepted: 10/01/2019] [Indexed: 02/07/2023]
Abstract
Hydrogels are water enriched soft materials widely used for applications as varied as super absorbents, breast implants and contact lenses. Hydrogels have also been designed for smart functional devices including drug delivery, tissue engineering and diagnostics such as blood typing. The hydrogel properties and functionality depend on their crosslinking density, water holding capacity and fibre/polymer composition, strength and internal structure. Determining these parameters and properties are challenging. This review presents the main characterisation methods providing both qualitative and quantitative information of the structures and compositions of hydrogel. The length scale of interest ranges from the nano to the micro scale and the techniques and results are analysed in relationship to the hydrogel macroscopic applications. The characterisation methods examined aim at quantifying swelling, mechanical strength, mesh size, bound and free water content, pore structure, chemical composition, strength of chemical bonds and mechanical strength. These hydrogel parameters enable us to understand the fundamental mechanisms of hydrogel formation, to control their structure and functionality, and to optimize and tailor specific hydrogel properties to engineer particular applications.
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26
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Force and Collective Epithelial Activities. ADVANCES IN EXPERIMENTAL MEDICINE AND BIOLOGY 2019. [PMID: 31612452 DOI: 10.1007/978-3-030-17593-1_3] [Citation(s) in RCA: 0] [Impact Index Per Article: 0] [Reference Citation Analysis] [Abstract] [Key Words] [Track Full Text] [Subscribe] [Scholar Register] [Indexed: 08/27/2023]
Abstract
Cells apply forces to their surroundings to perform basic biological activities, including division, adhesion, and migration. Similarly, cell populations in epithelial tissues coordinate forces in physiological processes of morphogenesis and repair. These activities are highly regulated to yield the correct development and function of the body. The modification of this order is at the onset of pathological events and malfunctions. Mechanical forces and their translation into biological signals are the focus of an emerging field of research, shaping as a central discipline in the study of life and gathering knowledge at the interface of engineering, physics, biology and medicine. Novel engineering methods are needed to complement the classic instruments developed by molecular biology, physics and medicine. These should enable the measurement of forces at the cellular and multicellular level, and at a temporal and spatial resolution which is fully compatible with the ranges experienced by cells in vivo.
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27
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Colin-York H, Javanmardi Y, Barbieri L, Li D, Korobchevskaya K, Guo Y, Hall C, Taylor A, Khuon S, Sheridan GK, Chew TL, Li D, Moeendarbary E, Fritzsche M. Spatiotemporally Super-Resolved Volumetric Traction Force Microscopy. NANO LETTERS 2019; 19:4427-4434. [PMID: 31199151 PMCID: PMC6628183 DOI: 10.1021/acs.nanolett.9b01196] [Citation(s) in RCA: 35] [Impact Index Per Article: 7.0] [Reference Citation Analysis] [Abstract] [Key Words] [MESH Headings] [Grants] [Track Full Text] [Subscribe] [Scholar Register] [Received: 03/22/2019] [Revised: 06/12/2019] [Indexed: 05/21/2023]
Abstract
Quantification of mechanical forces is a major challenge across biomedical sciences. Yet such measurements are essential to understanding the role of biomechanics in cell regulation and function. Traction force microscopy remains the most broadly applied force probing technology but typically restricts itself to single-plane two-dimensional quantifications with limited spatiotemporal resolution. Here, we introduce an enhanced force measurement technique combining 3D super-resolution fluorescence structural illumination microscopy and traction force microscopy (3D-SIM-TFM) offering increased spatiotemporal resolution, opening-up unprecedented insights into physiological three-dimensional force production in living cells.
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Affiliation(s)
- Huw Colin-York
- MRC
Human Immunology Unit, Weatherall Institute of Molecular Medicine, University of Oxford, Headley Way, Oxford OX3 9DS, United Kingdom
| | - Yousef Javanmardi
- Department
of Mechanical Engineering, University College
London, London WC1E 7JE, United Kingdom
| | - Liliana Barbieri
- MRC
Human Immunology Unit, Weatherall Institute of Molecular Medicine, University of Oxford, Headley Way, Oxford OX3 9DS, United Kingdom
| | - Di Li
- National
Laboratory of Biomacromolecules, Institute of Biophysics, Chinese Academy of Sciences, Beijing 100101, China
| | - Kseniya Korobchevskaya
- Kennedy
Institute for Rheumatology, University of
Oxford, Roosevelt Drive, Oxford OX3 7LF, United Kingdom
| | - Yuting Guo
- National
Laboratory of Biomacromolecules, Institute of Biophysics, Chinese Academy of Sciences, Beijing 100101, China
- College
of Life Sciences, University of Chinese
Academy of Sciences, Beijing 100049, China
| | - Chloe Hall
- Department
of Mechanical Engineering, University College
London, London WC1E 7JE, United Kingdom
| | - Aaron Taylor
- Howard Hughes
Medical Institute, Janelia Research Campus, 19700 Helix Drive, Ashburn, Virginia 20147, United States
| | - Satya Khuon
- Howard Hughes
Medical Institute, Janelia Research Campus, 19700 Helix Drive, Ashburn, Virginia 20147, United States
| | - Graham K. Sheridan
- School
of Pharmacy and Biomolecular Sciences, University
of Brighton, Brighton BN2 4AT, United Kingdom
| | - Teng-Leong Chew
- Howard Hughes
Medical Institute, Janelia Research Campus, 19700 Helix Drive, Ashburn, Virginia 20147, United States
| | - Dong Li
- National
Laboratory of Biomacromolecules, Institute of Biophysics, Chinese Academy of Sciences, Beijing 100101, China
- College
of Life Sciences, University of Chinese
Academy of Sciences, Beijing 100049, China
| | - Emad Moeendarbary
- Department
of Mechanical Engineering, University College
London, London WC1E 7JE, United Kingdom
- Department
of Biological Engineering, Massachusetts
Institute of Technology, Cambridge, Massachusetts 02139, United States
| | - Marco Fritzsche
- MRC
Human Immunology Unit, Weatherall Institute of Molecular Medicine, University of Oxford, Headley Way, Oxford OX3 9DS, United Kingdom
- Kennedy
Institute for Rheumatology, University of
Oxford, Roosevelt Drive, Oxford OX3 7LF, United Kingdom
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28
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Sao K, Jones TM, Doyle AD, Maity D, Schevzov G, Chen Y, Gunning PW, Petrie RJ. Myosin II governs intracellular pressure and traction by distinct tropomyosin-dependent mechanisms. Mol Biol Cell 2019; 30:1170-1181. [PMID: 30865560 PMCID: PMC6724525 DOI: 10.1091/mbc.e18-06-0355] [Citation(s) in RCA: 24] [Impact Index Per Article: 4.8] [Reference Citation Analysis] [Abstract] [Track Full Text] [Download PDF] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Indexed: 12/31/2022] Open
Abstract
Two-dimensional (2D) substrate rigidity promotes myosin II activity to increase traction force in a process negatively regulated by tropomyosin (Tpm) 2.1. We recently discovered that actomyosin contractility can increase intracellular pressure and switch tumor cells from low-pressure lamellipodia to high-pressure lobopodial protrusions during three-dimensional (3D) migration. However, it remains unclear whether these myosin II–generated cellular forces are produced simultaneously, and by the same molecular machinery. Here we identify Tpm 1.6 as a positive regulator of intracellular pressure and confirm that Tpm 2.1 is a negative regulator of traction force. We find that Tpm 1.6 and 2.1 can control intracellular pressure and traction independently, suggesting these myosin II–dependent forces are generated by distinct mechanisms. Further, these tropomyosin-regulated mechanisms can be integrated to control complex cell behaviors on 2D and in 3D environments.
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Affiliation(s)
- Kimheak Sao
- Department of Biology, Drexel University, Philadelphia, PA 19104
| | - Tia M Jones
- Department of Biology, Drexel University, Philadelphia, PA 19104
| | - Andrew D Doyle
- National Institute of Dental and Craniofacial Research, National Institutes of Health, Bethesda, MD 20892
| | - Debonil Maity
- Department of Mechanical Engineering, Johns Hopkins University, Baltimore, MD 21218
| | - Galina Schevzov
- School of Medical Sciences, University of New South Wales, Sydney NSW 2052, Australia
| | - Yun Chen
- Department of Mechanical Engineering, Johns Hopkins University, Baltimore, MD 21218
| | - Peter W Gunning
- School of Medical Sciences, University of New South Wales, Sydney NSW 2052, Australia
| | - Ryan J Petrie
- Department of Biology, Drexel University, Philadelphia, PA 19104
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29
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30
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Fernandez A, Bautista M, Stanciauskas R, Chung T, Pinaud F. Cell-Shaping Micropatterns for Quantitative Super-Resolution Microscopy Imaging of Membrane Mechanosensing Proteins. ACS APPLIED MATERIALS & INTERFACES 2017; 9:27575-27586. [PMID: 28766344 DOI: 10.1021/acsami.7b09743] [Citation(s) in RCA: 7] [Impact Index Per Article: 1.0] [Reference Citation Analysis] [Abstract] [Key Words] [MESH Headings] [Track Full Text] [Subscribe] [Scholar Register] [Indexed: 06/07/2023]
Abstract
Patterning cells on microcontact-printed substrates is a powerful approach to control cell morphology and introduce specific mechanical cues on a cell's molecular organization. Although global changes in cellular architectures caused by micropatterns can easily be probed with diffraction-limited optical microscopy, studying molecular reorganizations at the nanoscale demands micropatterned substrates that accommodate the optical requirements of single molecule microscopy techniques. Here, we developed a simple micropatterning strategy that provides control of cellular architectures and is optimized for nanometer accuracy single molecule tracking and three-dimensional super-resolution imaging of plasma and nuclear membrane proteins in cells. This approach, based on fibronectin microcontact printing on hydrophobic organosilane monolayers, allows evanescent wave and light-sheet microscopy of cells whilst fulfilling the stringent optical demands of point reconstruction optical microscopy. By imposing steady-state mechanical cues on cells grown in these micropatterns, we reveal nanoscale remodeling in the dynamics and the structural organizations of the nuclear envelope mechanotransducing protein emerin and of the plasma membrane mechanosensing protein caveolin-1 using single particle tracking photoactivated localization microscopy and direct stochastic optical reconstruction microscopy imaging. In addition to allowing quantitative biophysical studies of mechanoresponsive membrane proteins, this approach provides an easy means to probe mechanical regulations in cellular membranes with high optical resolution and nanometer precision.
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Affiliation(s)
- Anthony Fernandez
- Department of Biological Sciences, ‡Department of Chemistry, and §Department of Physics and Astronomy, University of Southern California , Los Angeles, California 90089, United States
| | - Markville Bautista
- Department of Biological Sciences, ‡Department of Chemistry, and §Department of Physics and Astronomy, University of Southern California , Los Angeles, California 90089, United States
| | - Ramunas Stanciauskas
- Department of Biological Sciences, ‡Department of Chemistry, and §Department of Physics and Astronomy, University of Southern California , Los Angeles, California 90089, United States
| | - Taerin Chung
- Department of Biological Sciences, ‡Department of Chemistry, and §Department of Physics and Astronomy, University of Southern California , Los Angeles, California 90089, United States
| | - Fabien Pinaud
- Department of Biological Sciences, ‡Department of Chemistry, and §Department of Physics and Astronomy, University of Southern California , Los Angeles, California 90089, United States
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31
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Yeh YC, Corbin EA, Caliari SR, Ouyang L, Vega SL, Truitt R, Han L, Margulies KB, Burdick JA. Mechanically dynamic PDMS substrates to investigate changing cell environments. Biomaterials 2017; 145:23-32. [PMID: 28843064 DOI: 10.1016/j.biomaterials.2017.08.033] [Citation(s) in RCA: 52] [Impact Index Per Article: 7.4] [Reference Citation Analysis] [Abstract] [Key Words] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Received: 05/30/2017] [Revised: 07/28/2017] [Accepted: 08/16/2017] [Indexed: 01/06/2023]
Abstract
Mechanics of the extracellular matrix (ECM) play a pivotal role in governing cell behavior, such as cell spreading and differentiation. ECM mechanics have been recapitulated primarily in elastic hydrogels, including with dynamic properties to mimic complex behaviors (e.g., fibrosis); however, these dynamic hydrogels fail to introduce the viscoelastic nature of many tissues. Here, we developed a two-step crosslinking strategy to first form (via platinum-catalyzed crosslinking) networks of polydimethylsiloxane (PDMS) and then to increase PDMS crosslinking (via thiol-ene click reaction) in a temporally-controlled manner. This photoinitiated reaction increased the compressive modulus of PDMS up to 10-fold within minutes and was conducted under cytocompatible conditions. With stiffening, cells displayed increased spreading, changing from ∼1300 to 1900 μm2 and from ∼2700 to 4600 μm2 for fibroblasts and mesenchymal stem cells, respectively. In addition, higher myofibroblast activation (from ∼2 to 20%) for cardiac fibroblasts was observed with increasing PDMS substrate stiffness. These results indicate a cellular response to changes in PDMS substrate mechanics, along with a demonstration of a mechanically dynamic and photoresponsive PDMS substrate platform to model the dynamic behavior of ECM.
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Affiliation(s)
- Yi-Cheun Yeh
- Department of Bioengineering, University of Pennsylvania, Philadelphia, PA, USA
| | - Elise A Corbin
- Cardiovascular Institute, University of Pennsylvania, Philadelphia, PA, USA
| | - Steven R Caliari
- Department of Bioengineering, University of Pennsylvania, Philadelphia, PA, USA
| | - Liu Ouyang
- School of Biomedical Engineering, Science and Health Systems, Drexel University, Philadelphia, PA, USA
| | - Sebastián L Vega
- Department of Bioengineering, University of Pennsylvania, Philadelphia, PA, USA
| | - Rachel Truitt
- Department of Bioengineering, University of Pennsylvania, Philadelphia, PA, USA; Cardiovascular Institute, University of Pennsylvania, Philadelphia, PA, USA
| | - Lin Han
- School of Biomedical Engineering, Science and Health Systems, Drexel University, Philadelphia, PA, USA
| | | | - Jason A Burdick
- Department of Bioengineering, University of Pennsylvania, Philadelphia, PA, USA.
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32
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Costigliola N, Ding L, Burckhardt CJ, Han SJ, Gutierrez E, Mota A, Groisman A, Mitchison TJ, Danuser G. Vimentin fibers orient traction stress. Proc Natl Acad Sci U S A 2017; 114:5195-5200. [PMID: 28465431 PMCID: PMC5441818 DOI: 10.1073/pnas.1614610114] [Citation(s) in RCA: 81] [Impact Index Per Article: 11.6] [Reference Citation Analysis] [Abstract] [Key Words] [MESH Headings] [Grants] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Indexed: 12/28/2022] Open
Abstract
The intermediate filament vimentin is required for cells to transition from the epithelial state to the mesenchymal state and migrate as single cells; however, little is known about the specific role of vimentin in the regulation of mesenchymal migration. Vimentin is known to have a significantly greater ability to resist stress without breaking in vitro compared with actin or microtubules, and also to increase cell elasticity in vivo. Therefore, we hypothesized that the presence of vimentin could support the anisotropic mechanical strain of single-cell migration. To study this, we fluorescently labeled vimentin with an mEmerald tag using TALEN genome editing. We observed vimentin architecture in migrating human foreskin fibroblasts and found that network organization varied from long, linear bundles, or "fibers," to shorter fragments with a mesh-like organization. We developed image analysis tools employing steerable filtering and iterative graph matching to characterize the fibers embedded in the surrounding mesh. Vimentin fibers were aligned with fibroblast branching and migration direction. The presence of the vimentin network was correlated with 10-fold slower local actin retrograde flow rates, as well as spatial homogenization of actin-based forces transmitted to the substrate. Vimentin fibers coaligned with and were required for the anisotropic orientation of traction stresses. These results indicate that the vimentin network acts as a load-bearing superstructure capable of integrating and reorienting actin-based forces. We propose that vimentin's role in cell motility is to govern the alignment of traction stresses that permit single-cell migration.
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Affiliation(s)
- Nancy Costigliola
- Department of Cell Biology, Harvard Medical School, Boston, MA 02115
- Department of Systems Biology, Harvard Medical School, Boston, MA 02115
| | - Liya Ding
- Department of Cell Biology, Harvard Medical School, Boston, MA 02115
- Department of Cell Biology, University of Texas Southwestern Medical Center at Dallas, Dallas, TX 75390
| | - Christoph J Burckhardt
- Department of Cell Biology, Harvard Medical School, Boston, MA 02115
- Department of Cell Biology, University of Texas Southwestern Medical Center at Dallas, Dallas, TX 75390
| | - Sangyoon J Han
- Department of Cell Biology, Harvard Medical School, Boston, MA 02115
- Department of Cell Biology, University of Texas Southwestern Medical Center at Dallas, Dallas, TX 75390
| | - Edgar Gutierrez
- Department of Physics, University of California, San Diego, La Jolla, CA 92093
| | - Andressa Mota
- Department of Cell Biology, Harvard Medical School, Boston, MA 02115
| | - Alex Groisman
- Department of Physics, University of California, San Diego, La Jolla, CA 92093
| | | | - Gaudenz Danuser
- Department of Cell Biology, Harvard Medical School, Boston, MA 02115;
- Department of Cell Biology, University of Texas Southwestern Medical Center at Dallas, Dallas, TX 75390
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33
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Cardoso Dos Santos M, Vézy C, Morjani H, Jaffol R. Single cell adhesion strength assessed with variable-angle total internal reflection fluorescence microscopy. AIMS BIOPHYSICS 2017. [DOI: 10.3934/biophy.2017.3.438] [Citation(s) in RCA: 4] [Impact Index Per Article: 0.6] [Reference Citation Analysis] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Indexed: 12/15/2022] Open
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34
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Ou G, Thakar D, Tung JC, Miroshnikova YA, Dufort CC, Gutierrez E, Groisman A, Weaver VM. Visualizing mechanical modulation of nanoscale organization of cell-matrix adhesions. Integr Biol (Camb) 2016; 8:795-804. [PMID: 27334548 PMCID: PMC4980125 DOI: 10.1039/c6ib00031b] [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] [Indexed: 01/14/2023]
Abstract
The mechanical properties of the extracellular matrix influence cell signaling to regulate key cellular processes, including differentiation, apoptosis, and transformation. Understanding the molecular mechanisms underlying mechanotransduction is contingent upon our ability to visualize the effect of altered matrix properties on the nanoscale organization of proteins involved in this signalling. The development of super-resolution imaging techniques has afforded researchers unprecedented ability to probe the organization and localization of proteins within the cell. However, most of these methods require use of substrates like glass or silicon wafers, which are artificially rigid. In light of a growing body of literature demonstrating the importance of mechanical properties of the extracellular matrix in regulating many aspects of cellular behavior and signaling, we have developed a system that allows scanning angle interference microscopy on a mechanically tunable substrate. We describe its implementation in detail and provide examples of how it may be used to aide investigations into the effect of substrate rigidity on intracellular signaling.
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Affiliation(s)
- Guanqing Ou
- University of California, Berkeley and University of California, San Francisco Joint Graduate Group in Bioengineering, San Francisco, CA, USA
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35
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Jorge-Peñas A, Izquierdo-Alvarez A, Aguilar-Cuenca R, Vicente-Manzanares M, Garcia-Aznar JM, Van Oosterwyck H, de-Juan-Pardo EM, Ortiz-de-Solorzano C, Muñoz-Barrutia A. Free Form Deformation-Based Image Registration Improves Accuracy of Traction Force Microscopy. PLoS One 2015; 10:e0144184. [PMID: 26641883 PMCID: PMC4671587 DOI: 10.1371/journal.pone.0144184] [Citation(s) in RCA: 21] [Impact Index Per Article: 2.3] [Reference Citation Analysis] [Abstract] [MESH Headings] [Track Full Text] [Download PDF] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Received: 08/19/2015] [Accepted: 11/13/2015] [Indexed: 01/08/2023] Open
Abstract
Traction Force Microscopy (TFM) is a widespread method used to recover cellular tractions from the deformation that they cause in their surrounding substrate. Particle Image Velocimetry (PIV) is commonly used to quantify the substrate’s deformations, due to its simplicity and efficiency. However, PIV relies on a block-matching scheme that easily underestimates the deformations. This is especially relevant in the case of large, locally non-uniform deformations as those usually found in the vicinity of a cell’s adhesions to the substrate. To overcome these limitations, we formulate the calculation of the deformation of the substrate in TFM as a non-rigid image registration process that warps the image of the unstressed material to match the image of the stressed one. In particular, we propose to use a B-spline -based Free Form Deformation (FFD) algorithm that uses a connected deformable mesh to model a wide range of flexible deformations caused by cellular tractions. Our FFD approach is validated in 3D fields using synthetic (simulated) data as well as with experimental data obtained using isolated endothelial cells lying on a deformable, polyacrylamide substrate. Our results show that FFD outperforms PIV providing a deformation field that allows a better recovery of the magnitude and orientation of tractions. Together, these results demonstrate the added value of the FFD algorithm for improving the accuracy of traction recovery.
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Affiliation(s)
- Alvaro Jorge-Peñas
- Biomechanics Section, Department of Mechanical Engineering, KU Leuven, 3001, Leuven, Belgium
| | | | - Rocio Aguilar-Cuenca
- Instituto de Investigación Sanitaria-Hospital Universitario de la Princesa, Universidad Autonoma de Madrid, School of Medicine, 28006, Madrid, Spain
| | - Miguel Vicente-Manzanares
- Instituto de Investigación Sanitaria-Hospital Universitario de la Princesa, Universidad Autonoma de Madrid, School of Medicine, 28006, Madrid, Spain
| | - José Manuel Garcia-Aznar
- Multiscale in Mechanical and Biological Engineering (M2BE), Department of Mechanical Engineering, Aragon Institute of Engineering Research (I3A), University of Zaragoza, 50018, Zaragoza, Spain
| | - Hans Van Oosterwyck
- Biomechanics Section, Department of Mechanical Engineering, KU Leuven, 3001, Leuven, Belgium
- Prometheus, Division of Skeletal Tissue Engineering, KU Leuven, Leuven, Belgium
| | - Elena M. de-Juan-Pardo
- Regenerative Medicine Program, Institute of Health and Biomedical Innovation, Queensland University of Technology, 4059, Brisbane, Australia
| | - Carlos Ortiz-de-Solorzano
- Cancer Imaging Laboratory, Program in Solid Tumors and Biomarkers, Center for Applied Medical Research (CIMA), University of Navarra, Navarra’s Health Research Institute (IDISNA), 31008, Pamplona, Spain
| | - Arrate Muñoz-Barrutia
- Bioengineering and Aerospace Engineering Department, Universidad Carlos III de Madrid, Instituto de Investigación Sanitaria Gregorio Marañon, 28911, Madrid, Spain
- * E-mail:
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36
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Schwarz US, Soiné JR. Traction force microscopy on soft elastic substrates: A guide to recent computational advances. BIOCHIMICA ET BIOPHYSICA ACTA-MOLECULAR CELL RESEARCH 2015; 1853:3095-104. [DOI: 10.1016/j.bbamcr.2015.05.028] [Citation(s) in RCA: 101] [Impact Index Per Article: 11.2] [Reference Citation Analysis] [Track Full Text] [Subscribe] [Scholar Register] [Received: 03/16/2015] [Revised: 05/21/2015] [Accepted: 05/22/2015] [Indexed: 10/24/2022]
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37
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Lee K, Elliott HL, Oak Y, Zee CT, Groisman A, Tytell JD, Danuser G. Functional hierarchy of redundant actin assembly factors revealed by fine-grained registration of intrinsic image fluctuations. Cell Syst 2015; 1:37-50. [PMID: 26273703 DOI: 10.1016/j.cels.2015.07.001] [Citation(s) in RCA: 43] [Impact Index Per Article: 4.8] [Reference Citation Analysis] [Abstract] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Indexed: 01/19/2023]
Abstract
Highly redundant pathways often contain components whose functions are difficult to decipher from the responses induced by genetic or molecular perturbations. Here, we present a statistical approach that samples and registers events observed in images of intrinsic fluctuations in unperturbed cells to establish the functional hierarchy of events in systems with redundant pathways. We apply this approach to study the recruitment of actin assembly factors involved in the protrusion of the cell membrane. We find that the formin mDia1, along with nascent adhesion components, is recruited to the leading edge of the cell before protrusion onset, initiating linear growth of the lamellipodial network. Recruitment of Arp2/3, VASP, cofilin, and the formin mDia2 then promotes sustained exponential growth of the network. Experiments changing membrane tension suggest that Arp2/3 recruitment is mechano-responsive. These results indicate that cells adjust the overlapping contributions of multiple factors to actin filament assembly during protrusion on a ten-second timescale and in response to mechanical cues.
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Affiliation(s)
- Kwonmoo Lee
- Department of Cell Biology, Harvard Medical School, Boston, Massachusetts, 02115, USA
| | - Hunter L Elliott
- Department of Cell Biology, Harvard Medical School, Boston, Massachusetts, 02115, USA
| | - Youbean Oak
- Department of Cell Biology, Harvard Medical School, Boston, Massachusetts, 02115, USA
| | - Chih-Te Zee
- Department of Physics, University of California San Diego, La Jolla, California, 92093, USA
| | - Alex Groisman
- Department of Physics, University of California San Diego, La Jolla, California, 92093, USA
| | - Jessica D Tytell
- Department of Cell Biology, Harvard Medical School, Boston, Massachusetts, 02115, USA
| | - Gaudenz Danuser
- Department of Cell Biology, Harvard Medical School, Boston, Massachusetts, 02115, USA
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38
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Han SJ, Oak Y, Groisman A, Danuser G. Traction microscopy to identify force modulation in subresolution adhesions. Nat Methods 2015; 12:653-6. [PMID: 26030446 PMCID: PMC4490115 DOI: 10.1038/nmeth.3430] [Citation(s) in RCA: 108] [Impact Index Per Article: 12.0] [Reference Citation Analysis] [Abstract] [MESH Headings] [Grants] [Track Full Text] [Download PDF] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Received: 12/12/2014] [Accepted: 03/27/2015] [Indexed: 12/19/2022]
Abstract
We present a reconstruction algorithm that resolves cellular tractions in diffraction-limited nascent adhesions (NAs). The enabling method is the introduction of sparsity regularization to the solution of the inverse problem, which suppresses noise without underestimating traction magnitude. We show that NAs transmit a distinguishable amount of traction and that NA maturation depends on traction growth rate. A software package implementing this numerical approach is provided.
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Affiliation(s)
- Sangyoon J Han
- 1] Department of Cell Biology, Harvard Medical School, Boston, Massachusetts, USA. [2] Department of Cell Biology, University of Texas Southwestern Medical Center, Dallas, Texas, USA
| | - Youbean Oak
- Department of Cell Biology, Harvard Medical School, Boston, Massachusetts, USA
| | - Alex Groisman
- Department of Physics, University of California, San Diego, La Jolla, California, USA
| | - Gaudenz Danuser
- 1] Department of Cell Biology, Harvard Medical School, Boston, Massachusetts, USA. [2] Department of Cell Biology, University of Texas Southwestern Medical Center, Dallas, Texas, USA
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Nam KH, Jamilpour N, Mfoumou E, Wang FY, Zhang DD, Wong PK. Probing mechanoregulation of neuronal differentiation by plasma lithography patterned elastomeric substrates. Sci Rep 2014; 4:6965. [PMID: 25376886 PMCID: PMC4223667 DOI: 10.1038/srep06965] [Citation(s) in RCA: 25] [Impact Index Per Article: 2.5] [Reference Citation Analysis] [Abstract] [Track Full Text] [Download PDF] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Received: 09/09/2014] [Accepted: 10/22/2014] [Indexed: 01/14/2023] Open
Abstract
Cells sense and interpret mechanical cues, including cell-cell and cell-substrate interactions, in the microenvironment to collectively regulate various physiological functions. Understanding the influences of these mechanical factors on cell behavior is critical for fundamental cell biology and for the development of novel strategies in regenerative medicine. Here, we demonstrate plasma lithography patterning on elastomeric substrates for elucidating the influences of mechanical cues on neuronal differentiation and neuritogenesis. The neuroblastoma cells form neuronal spheres on plasma-treated regions, which geometrically confine the cells over two weeks. The elastic modulus of the elastomer is controlled simultaneously by the crosslinker concentration. The cell-substrate mechanical interactions are also investigated by controlling the size of neuronal spheres with different cell seeding densities. These physical cues are shown to modulate with the formation of focal adhesions, neurite outgrowth, and the morphology of neuroblastoma. By systematic adjustment of these cues, along with computational biomechanical analysis, we demonstrate the interrelated mechanoregulatory effects of substrate elasticity and cell size. Taken together, our results reveal that the neuronal differentiation and neuritogenesis of neuroblastoma cells are collectively regulated via the cell-substrate mechanical interactions.
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Affiliation(s)
- Ki-Hwan Nam
- 1] Department of Aerospace and Mechanical Engineering, The University of Arizona, Tucson, Arizona 85721, USA [2] Centre for Analytical Instrumentation Development, The Korea Basic Science Institute, Deajeon305-806, Korea
| | - Nima Jamilpour
- Department of Aerospace and Mechanical Engineering, The University of Arizona, Tucson, Arizona 85721, USA
| | - Etienne Mfoumou
- Department of Aerospace and Mechanical Engineering, The University of Arizona, Tucson, Arizona 85721, USA
| | - Fei-Yue Wang
- The Key Laboratory for Complex Systems and Intelligence Science, The Institute of Automation, Chinese Academy of Sciences, Beijing, China
| | - Donna D Zhang
- Department of Pharmacology and Toxicology, The University of Arizona, Tucson, Arizona. 85721, USA
| | - Pak Kin Wong
- Department of Aerospace and Mechanical Engineering, The University of Arizona, Tucson, Arizona 85721, USA
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Stretch-activated ion channel Piezo1 directs lineage choice in human neural stem cells. Proc Natl Acad Sci U S A 2014; 111:16148-53. [PMID: 25349416 DOI: 10.1073/pnas.1409802111] [Citation(s) in RCA: 392] [Impact Index Per Article: 39.2] [Reference Citation Analysis] [Abstract] [Key Words] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Indexed: 12/20/2022] Open
Abstract
Neural stem cells are multipotent cells with the ability to differentiate into neurons, astrocytes, and oligodendrocytes. Lineage specification is strongly sensitive to the mechanical properties of the cellular environment. However, molecular pathways transducing matrix mechanical cues to intracellular signaling pathways linked to lineage specification remain unclear. We found that the mechanically gated ion channel Piezo1 is expressed by brain-derived human neural stem/progenitor cells and is responsible for a mechanically induced ionic current. Piezo1 activity triggered by traction forces elicited influx of Ca(2+), a known modulator of differentiation, in a substrate-stiffness-dependent manner. Inhibition of channel activity by the pharmacological inhibitor GsMTx-4 or by siRNA-mediated Piezo1 knockdown suppressed neurogenesis and enhanced astrogenesis. Piezo1 knockdown also reduced the nuclear localization of the mechanoreactive transcriptional coactivator Yes-associated protein. We propose that the mechanically gated ion channel Piezo1 is an important determinant of mechanosensitive lineage choice in neural stem cells and may play similar roles in other multipotent stem cells.
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41
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Mettlen M, Danuser G. Imaging and modeling the dynamics of clathrin-mediated endocytosis. Cold Spring Harb Perspect Biol 2014; 6:a017038. [PMID: 25167858 DOI: 10.1101/cshperspect.a017038] [Citation(s) in RCA: 37] [Impact Index Per Article: 3.7] [Reference Citation Analysis] [Abstract] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Indexed: 12/21/2022]
Abstract
Clathrin-mediated endocytosis (CME) plays a central role in cellular homeostasis and is mediated by clathrin-coated pits (CCPs). Live-cell imaging has revealed a remarkable heterogeneity in CCP assembly kinetics, which can be used as an intrinsic source of mechanistic information on CCP regulation but also poses several major problems for unbiased analysis of CME dynamics. The backbone of unveiling the molecular control of CME is an imaging-based inventory of the full diversity of individual CCP behaviors, which requires detection and tracking of structural fiduciaries and regulatory proteins with an accuracy of >99.9%, despite very low signals. This level of confidence can only be achieved by combining appropriate imaging modalities with self-diagnostic computational algorithms for image analysis and data mining.
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Affiliation(s)
- Marcel Mettlen
- Department of Cell Biology, University of Texas Southwestern Medical Center, Dallas, Texas 75235-9039
| | - Gaudenz Danuser
- Department of Cell Biology, Harvard Medical School, Boston, Massachusetts 02115
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42
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Tseng P, Pushkarsky I, Di Carlo D. Metallization and biopatterning on ultra-flexible substrates via dextran sacrificial layers. PLoS One 2014; 9:e106091. [PMID: 25153326 PMCID: PMC4143360 DOI: 10.1371/journal.pone.0106091] [Citation(s) in RCA: 19] [Impact Index Per Article: 1.9] [Reference Citation Analysis] [Abstract] [MESH Headings] [Grants] [Track Full Text] [Download PDF] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Received: 04/04/2014] [Accepted: 07/31/2014] [Indexed: 11/23/2022] Open
Abstract
Micro-patterning tools adopted from the semiconductor industry have mostly been optimized to pattern features onto rigid silicon and glass substrates, however, recently the need to pattern on soft substrates has been identified in simulating cellular environments or developing flexible biosensors. We present a simple method of introducing a variety of patterned materials and structures into ultra-flexible polydimethylsiloxane (PDMS) layers (elastic moduli down to 3 kPa) utilizing water-soluble dextran sacrificial thin films. Dextran films provided a stable template for photolithography, metal deposition, particle adsorption, and protein stamping. These materials and structures (including dextran itself) were then readily transferrable to an elastomer surface following PDMS (10 to 70∶1 base to crosslinker ratios) curing over the patterned dextran layer and after sacrificial etch of the dextran in water. We demonstrate that this simple and straightforward approach can controllably manipulate surface wetting and protein adsorption characteristics of PDMS, covalently link protein patterns for stable cell patterning, generate composite structures of epoxy or particles for study of cell mechanical response, and stably integrate certain metals with use of vinyl molecular adhesives. This method is compatible over the complete moduli range of PDMS, and potentially generalizable over a host of additional micro- and nano-structures and materials.
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Affiliation(s)
- Peter Tseng
- Department of Bioengineering, University of California Los Angeles, Los Angeles, California, United States of America
| | - Ivan Pushkarsky
- Department of Bioengineering, University of California Los Angeles, Los Angeles, California, United States of America
| | - Dino Di Carlo
- Department of Bioengineering, University of California Los Angeles, Los Angeles, California, United States of America
- * E-mail:
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43
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Style RW, Boltyanskiy R, German GK, Hyland C, MacMinn CW, Mertz AF, Wilen LA, Xu Y, Dufresne ER. Traction force microscopy in physics and biology. SOFT MATTER 2014; 10:4047-55. [PMID: 24740485 DOI: 10.1039/c4sm00264d] [Citation(s) in RCA: 186] [Impact Index Per Article: 18.6] [Reference Citation Analysis] [Abstract] [MESH Headings] [Track Full Text] [Subscribe] [Scholar Register] [Indexed: 05/02/2023]
Abstract
Adherent cells, crawling slugs, peeling paint, sessile liquid drops, bearings and many other living and non-living systems apply forces to solid substrates. Traction force microscopy (TFM) provides spatially-resolved measurements of interfacial forces through the quantification and analysis of the deformation of an elastic substrate. Although originally developed for adherent cells, TFM has no inherent size or force scale, and can be applied to a much broader range of mechanical systems across physics and biology. In this paper, we showcase the wide range of applicability of TFM, describe the theory, and provide experimental details and code so that experimentalists can rapidly adopt this powerful technique.
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Liu K, Yuan Y, Huang J, Wei Q, Pang M, Xiong C, Fang J. Improved-throughput traction microscopy based on fluorescence micropattern for manual microscopy. PLoS One 2013; 8:e70122. [PMID: 23936383 PMCID: PMC3731345 DOI: 10.1371/journal.pone.0070122] [Citation(s) in RCA: 9] [Impact Index Per Article: 0.8] [Reference Citation Analysis] [Abstract] [MESH Headings] [Track Full Text] [Download PDF] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Received: 01/18/2013] [Accepted: 06/17/2013] [Indexed: 02/05/2023] Open
Abstract
Traction force microscopy (TFM) is a quantitative technique for measuring cellular traction force, which is important in understanding cellular mechanotransduction processes. Traditional TFM has a significant limitation in that it has a low measurement throughput, commonly one per TFM dish, due to a lack of cell position information. To obtain enough cellular traction force data, an onerous workload is required including numerous TFM dish preparations and heavy cell-seeding activities, creating further difficulty in achieving identical experimental conditions among batches. In this paper, we present an improved-throughput TFM method using the well-developed microcontact printing technique and chemical modifications of linking microbeads to the gel surface to address these limitations. Chemically linking the microbeads to the gel surface has no significant influence on cell proliferation, morphology, cytoskeleton, and adhesion. Multiple pairs of force loaded and null force fluorescence images can be easily acquired by means of manual microscope with the aid of a fluorescence micropattern made by microcontact printing. Furthermore, keeping the micropattern separate from cells by using gels effectively eliminates the potential negative effect of the micropattern on the cells. This novel design greatly improves the analysis throughput of traditional TFM from one to at least twenty cells per petri dish without losing unique advantages, including a high spatial resolution of traction measurements. This newly developed method will boost the investigation of cell-matrix mechanical interactions.
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Affiliation(s)
- Kai Liu
- Academy for Advanced Interdisciplinary Studies, Peking University, Beijing, China
| | - Yuan Yuan
- Department of Mechanics and Aerospace Engineering, College of Engineering, Peking University, Beijing, China
| | - Jianyong Huang
- Academy for Advanced Interdisciplinary Studies, Peking University, Beijing, China
- Department of Mechanics and Aerospace Engineering, College of Engineering, Peking University, Beijing, China
| | - Qiong Wei
- Department of Mechanics and Aerospace Engineering, College of Engineering, Peking University, Beijing, China
| | - Mingshu Pang
- Department of Mechanics and Aerospace Engineering, College of Engineering, Peking University, Beijing, China
| | - Chunyang Xiong
- Academy for Advanced Interdisciplinary Studies, Peking University, Beijing, China
- Department of Mechanics and Aerospace Engineering, College of Engineering, Peking University, Beijing, China
- * E-mail:
| | - Jing Fang
- Academy for Advanced Interdisciplinary Studies, Peking University, Beijing, China
- Department of Mechanics and Aerospace Engineering, College of Engineering, Peking University, Beijing, China
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Sugihara K, Delai M, Mahnna R, Kusch J, Poulikakos D, Vörös J, Zambelli T, Ferrari A. Label-free detection of cell-contractile activity with lipid nanotubes. Integr Biol (Camb) 2012; 5:423-30. [DOI: 10.1039/c2ib20202f] [Citation(s) in RCA: 6] [Impact Index Per Article: 0.5] [Reference Citation Analysis] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Indexed: 01/16/2023]
Affiliation(s)
- Kaori Sugihara
- Laboratory of Biosensors and Bioelectronics, Institute for Biomedical Engineering, ETH Zurich, Gloriastrasse 35, CH-8092 Zurich, Switzerland
| | - Marco Delai
- Laboratory of Biosensors and Bioelectronics, Institute for Biomedical Engineering, ETH Zurich, Gloriastrasse 35, CH-8092 Zurich, Switzerland
| | - Rami Mahnna
- Laboratory of Biosensors and Bioelectronics, Institute for Biomedical Engineering, ETH Zurich, Gloriastrasse 35, CH-8092 Zurich, Switzerland
| | - Justine Kusch
- LMC, Switzerland Light Microscopy Center, D-Biol, ETH Zurich, Schafmattstrasse 18, CH-8093 Zurich, Switzerland
| | - Dimos Poulikakos
- Laboratory of Thermodynamics in Emerging Technologies, Institute of Energy Technology, Department of Mechanical and Process Engineering, ETH Zurich, Sonneggstrasse 3, CH-8092 Zurich, Switzerland
| | - János Vörös
- Laboratory of Biosensors and Bioelectronics, Institute for Biomedical Engineering, ETH Zurich, Gloriastrasse 35, CH-8092 Zurich, Switzerland
| | - Tomaso Zambelli
- Laboratory of Biosensors and Bioelectronics, Institute for Biomedical Engineering, ETH Zurich, Gloriastrasse 35, CH-8092 Zurich, Switzerland
| | - Aldo Ferrari
- Laboratory of Thermodynamics in Emerging Technologies, Institute of Energy Technology, Department of Mechanical and Process Engineering, ETH Zurich, Sonneggstrasse 3, CH-8092 Zurich, Switzerland
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Gutierrez E, Groisman A. Measurements of elastic moduli of silicone gel substrates with a microfluidic device. PLoS One 2011; 6:e25534. [PMID: 21980487 PMCID: PMC3184124 DOI: 10.1371/journal.pone.0025534] [Citation(s) in RCA: 48] [Impact Index Per Article: 3.7] [Reference Citation Analysis] [Abstract] [MESH Headings] [Grants] [Track Full Text] [Download PDF] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Received: 04/26/2011] [Accepted: 09/07/2011] [Indexed: 11/19/2022] Open
Abstract
Thin layers of gels with mechanical properties mimicking animal tissues are widely used to study the rigidity sensing of adherent animal cells and to measure forces applied by cells to their substrate with traction force microscopy. The gels are usually based on polyacrylamide and their elastic modulus is measured with an atomic force microscope (AFM). Here we present a simple microfluidic device that generates high shear stresses in a laminar flow above a gel-coated substrate and apply the device to gels with elastic moduli in a range from 0.4 to 300 kPa that are all prepared by mixing two components of a transparent commercial silicone Sylgard 184. The elastic modulus is measured by tracking beads on the gel surface under a wide-field fluorescence microscope without any other specialized equipment. The measurements have small and simple to estimate errors and their results are confirmed by conventional tensile tests. A master curve is obtained relating the mixing ratios of the two components of Sylgard 184 with the resulting elastic moduli of the gels. The rigidity of the silicone gels is less susceptible to effects from drying, swelling, and aging than polyacrylamide gels and can be easily coated with fluorescent tracer particles and with molecules promoting cellular adhesion. This work can lead to broader use of silicone gels in the cell biology laboratory and to improved repeatability and accuracy of cell traction force microscopy and rigidity sensing experiments.
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Affiliation(s)
- Edgar Gutierrez
- Department of Physics, University of California San Diego, La Jolla, California, United States of America
| | - Alex Groisman
- Department of Physics, University of California San Diego, La Jolla, California, United States of America
- * E-mail:
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