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Wiegel J, Helmstädter M, Walz G, Bergen MD. Spontaneous Calcium Bursts Organize the Apical Actin Cytoskeleton of Multiciliated Cells. Int J Mol Sci 2025; 26:2507. [PMID: 40141151 PMCID: PMC11942550 DOI: 10.3390/ijms26062507] [Citation(s) in RCA: 0] [Impact Index Per Article: 0] [Reference Citation Analysis] [Abstract] [Key Words] [MESH Headings] [Grants] [Track Full Text] [Download PDF] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Received: 02/03/2025] [Revised: 03/05/2025] [Accepted: 03/07/2025] [Indexed: 03/28/2025] Open
Abstract
Motile cilia perform crucial functions during embryonic development and in adult tissues. They are anchored by an apical actin network that forms microridge-like structures on the surface of multiciliated cells. Using Xenopus as a model system to investigate the mechanisms underlying the formation of these specialized actin structures, we observed stochastic bursts of intracellular calcium concentration in developing multiciliated cells. Through optogenetic manipulation of calcium signaling, we found that individual calcium bursts triggered the fusion and extension of actin structures by activating non-muscle myosin. Repeated cycles of calcium activation promoted assembly and coherence of the maturing apical actin network. Inhibition of the endogenous inositol triphosphate-calcium pathway disrupted the formation of apical actin/microridge-like structures by reducing local centriolar RhoA signaling. This disruption was rescued by transient expression of constitutively active RhoA in multiciliated cells. Our findings identify repetitive calcium bursts as a driving force that promotes the self-organization of the highly specialized actin cytoskeleton of multiciliated cells.
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Affiliation(s)
- Johannes Wiegel
- Department of Medicine IV, University Freiburg Medical Center, Faculty of Medicine, University of Freiburg, Hugstetter Strasse 55, 79106 Freiburg, Germany; (J.W.); (M.H.); (G.W.)
| | - Martin Helmstädter
- Department of Medicine IV, University Freiburg Medical Center, Faculty of Medicine, University of Freiburg, Hugstetter Strasse 55, 79106 Freiburg, Germany; (J.W.); (M.H.); (G.W.)
- EMcore, Renal Division, Department of Medicine, University Freiburg Medical Center, Faculty of Medicine, University of Freiburg, 79106 Freiburg, Germany
| | - Gerd Walz
- Department of Medicine IV, University Freiburg Medical Center, Faculty of Medicine, University of Freiburg, Hugstetter Strasse 55, 79106 Freiburg, Germany; (J.W.); (M.H.); (G.W.)
- BIOSS and CIBSS Centre for Integrative Biological Signalling, University of Freiburg, Schänzlestrasse 18, 79104 Freiburg, Germany
| | - Max D. Bergen
- Department of Medicine IV, University Freiburg Medical Center, Faculty of Medicine, University of Freiburg, Hugstetter Strasse 55, 79106 Freiburg, Germany; (J.W.); (M.H.); (G.W.)
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2
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Ansel M, Ramachandran K, Dey G, Brunet T. Origin and evolution of microvilli. Biol Cell 2024; 116:e2400054. [PMID: 39233537 DOI: 10.1111/boc.202400054] [Citation(s) in RCA: 0] [Impact Index Per Article: 0] [Reference Citation Analysis] [Abstract] [Key Words] [MESH Headings] [Grants] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Received: 05/17/2024] [Revised: 07/31/2024] [Accepted: 08/13/2024] [Indexed: 09/06/2024]
Abstract
BACKGROUND INFORMATION Microvilli are finger-like, straight, and stable cellular protrusions that are filled with F-actin and present a stereotypical length. They are present in a broad range of cell types across the animal tree of life and mediate several fundamental functions, including nutrient absorption, photosensation, and mechanosensation. Therefore, understanding the origin and evolution of microvilli is key to reconstructing the evolution of animal cellular form and function. Here, we review the current state of knowledge on microvilli evolution and perform a bioinformatic survey of the conservation of genes encoding microvillar proteins in animals and their unicellular relatives. RESULTS We first present a detailed description of mammalian microvilli based on two well-studied examples, the brush border microvilli of enterocytes and the stereocilia of hair cells. We also survey the broader diversity of microvilli and discuss similarities and differences between microvilli and filopodia. Based on our bioinformatic survey coupled with carefully reconstructed molecular phylogenies, we reconstitute the order of evolutionary appearance of microvillar proteins. We document the stepwise evolutionary assembly of the "molecular microvillar toolkit" with notable bursts of innovation at two key nodes: the last common filozoan ancestor (correlated with the evolution of microvilli distinct from filopodia) and the last common choanozoan ancestor (correlated with the emergence of inter-microvillar adhesions). CONCLUSION AND SIGNIFICANCE We conclude with a scenario for the evolution of microvilli from filopodia-like ancestral structures in unicellular precursors of animals.
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Affiliation(s)
- Mylan Ansel
- Institut Pasteur, Université Paris-Cité, CNRS UMR3691, Evolutionary Cell Biology and Evolution of Morphogenesis Unit, Paris, France
- Cell Biology and Biophysics, European Molecular Biology Laboratory, Heidelberg, Germany
- Master BioSciences, Département de Biologie, Ecole Normale Supérieure de Lyon, Lyon, France
| | - Kaustubh Ramachandran
- Cell Biology and Biophysics, European Molecular Biology Laboratory, Heidelberg, Germany
| | - Gautam Dey
- Cell Biology and Biophysics, European Molecular Biology Laboratory, Heidelberg, Germany
| | - Thibaut Brunet
- Institut Pasteur, Université Paris-Cité, CNRS UMR3691, Evolutionary Cell Biology and Evolution of Morphogenesis Unit, Paris, France
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3
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Rheinlaender J, Schäffer TE. Measuring the Shape, Stiffness, and Interface Tension of Droplets with the Scanning Ion Conductance Microscope. ACS NANO 2024; 18:16257-16264. [PMID: 38868865 DOI: 10.1021/acsnano.4c02743] [Citation(s) in RCA: 0] [Impact Index Per Article: 0] [Reference Citation Analysis] [Abstract] [Key Words] [Track Full Text] [Subscribe] [Scholar Register] [Indexed: 06/14/2024]
Abstract
Imaging and probing liquid-liquid interfaces at the micro- and nanoscale are of high relevance, for example, in materials science, surface chemistry, and microfluidics. However, existing imaging techniques are limited in resolution, average over large sample areas, or interact with the sample. Here, we present a method to quantify the shape, stiffness, and interface tension of liquid droplets with the scanning ion conductance microscope (SICM), providing submicrometer resolution and the ability to perform noncontact mechanical measurements. We show that we can accurately image the three-dimensional shape of micrometer-sized liquid droplets made of, for example, decane, hexane, or different oils. We then introduce numerical models to quantitatively obtain their stiffness and interface tension from SICM data. We verified our method by measuring the interface tension of decane droplets changing under the influence of surfactants at different concentrations. Finally, we use SICM to resolve the dissolution dynamics of decane droplets, showing that droplet shape exhibits different dissolution modes and stiffness continuously increases while the interface tension remains constant. We thereby demonstrate that SICM is a useful method to investigate liquid-liquid interfaces on the microscale with applications in materials or life sciences.
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Affiliation(s)
- Johannes Rheinlaender
- Institute of Applied Physics, University of Tübingen, Auf der Morgenstelle 10, Tübingen, Tübingen 72076, Germany
| | - Tilman E Schäffer
- Institute of Applied Physics, University of Tübingen, Auf der Morgenstelle 10, Tübingen, Tübingen 72076, Germany
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4
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Muhammed Y, Lazenby RA. Scanning ion conductance microscopy revealed cisplatin-induced morphological changes related to apoptosis in single adenocarcinoma cells. ANALYTICAL METHODS : ADVANCING METHODS AND APPLICATIONS 2024; 16:503-514. [PMID: 38167666 DOI: 10.1039/d3ay01827j] [Citation(s) in RCA: 0] [Impact Index Per Article: 0] [Reference Citation Analysis] [Abstract] [MESH Headings] [Track Full Text] [Subscribe] [Scholar Register] [Indexed: 01/05/2024]
Abstract
The studies of drug-induced apoptosis play a vital role in the identification of potential drugs that could treat diseases such as cancer. Alterations in the native morphology of cancer cells following treatment with anticancer drugs serve as one of the indicators that reveal drug efficacy. Various techniques such as optical microscopy, electron microscopy (EM), and atomic force microscopy (AFM) have been used to map the three dimensional (3D) morphological changes in cells induced with drugs. However, caution should be exercised when interpreting morphological data from techniques that might alter the native morphology of cells, caused by phototoxicity, electron beam invasiveness, intrusive sample preparation, and cell membrane deformation. Herein, we have used scanning ion conductance microscopy (SICM) to study the 3D morphology and roughness of A549 adenocarcinoma cells under physiological conditions before and after cisplatin induced apoptosis, where we observed an increase in height, overall shrinkage of the cells, and irregular features form on the cell membrane. Tracking the morphology of the same single A549 cells exposed to cisplatin unveiled heterogeneity in response to the drug, formation of membrane blebs, and an increase in membrane roughness. We have also demonstrated the use of SICM for studying the effect of cisplatin on the dynamic changes in the volume of A549 cells over days. SICM is demonstrated as a technique for studying the effect of drug induced apoptosis in the same cells over time, and for multiple different single cells.
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Affiliation(s)
- Yusuf Muhammed
- Department of Chemistry and Biochemistry, Florida State University, Tallahassee, Florida 32306-4390, USA.
| | - Robert A Lazenby
- Department of Chemistry and Biochemistry, Florida State University, Tallahassee, Florida 32306-4390, USA.
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5
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Zhang H, Jiang H, Liu X, Wang X. A review of innovative electrochemical strategies for bioactive molecule detection and cell imaging: Current advances and challenges. Anal Chim Acta 2024; 1285:341920. [PMID: 38057043 DOI: 10.1016/j.aca.2023.341920] [Citation(s) in RCA: 0] [Impact Index Per Article: 0] [Reference Citation Analysis] [Abstract] [Key Words] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Received: 09/12/2023] [Revised: 10/13/2023] [Accepted: 10/14/2023] [Indexed: 12/08/2023]
Abstract
Cellular heterogeneity poses a major challenge for tumor theranostics, requiring high-resolution intercellular bioanalysis strategies. Over the past decades, the advantages of electrochemical analysis, such as high sensitivity, good spatio-temporal resolution, and ease of use, have made it the preferred method to uncover cellular differences. To inspire more creative research, herein, we highlight seminal works in electrochemical techniques for biomolecule analysis and bioimaging. Specifically, micro/nano-electrode-based electrochemical techniques enable real-time quantitative analysis of electroactive substances relevant to life processes in the micro-nanostructure of cells and tissues. Nanopore-based technique plays a vital role in biosensing by utilizing nanoscale pores to achieve high-precision detection and analysis of biomolecules with exceptional sensitivity and single-molecule resolution. Electrochemiluminescence (ECL) technology is utilized for real-time monitoring of the behavior and features of individual cancer cells, enabling observation of their dynamic processes due to its capability of providing high-resolution and highly sensitive bioimaging of cells. Particularly, scanning electrochemical microscopy (SECM) and scanning ion conductance microscopy (SICM) which are widely used in real-time observation of cell surface biological processes and three-dimensional imaging of micro-nano structures, such as metabolic activity, ion channel activity, and cell morphology are introduced in this review. Furthermore, the expansion of the scope of cellular electrochemistry research by innovative functionalized electrodes and electrochemical imaging models and strategies to address future challenges and potential applications is also discussed in this review.
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Affiliation(s)
- Hao Zhang
- State Key Laboratory of Digital Medical Engineering, School of Biological Science and Medical Engineering, Southeast University, Nanjing, Jiangsu 210096, China
| | - Hui Jiang
- State Key Laboratory of Digital Medical Engineering, School of Biological Science and Medical Engineering, Southeast University, Nanjing, Jiangsu 210096, China
| | - Xiaohui Liu
- State Key Laboratory of Digital Medical Engineering, School of Biological Science and Medical Engineering, Southeast University, Nanjing, Jiangsu 210096, China.
| | - Xuemei Wang
- State Key Laboratory of Digital Medical Engineering, School of Biological Science and Medical Engineering, Southeast University, Nanjing, Jiangsu 210096, China.
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6
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Kapustina M, Li D, Zhu J, Wall B, Weinreb V, Cheney RE. Changes in cell surface excess are coordinated with protrusion dynamics during 3D motility. Biophys J 2023; 122:3656-3677. [PMID: 37207658 PMCID: PMC10541482 DOI: 10.1016/j.bpj.2023.04.023] [Citation(s) in RCA: 0] [Impact Index Per Article: 0] [Reference Citation Analysis] [Abstract] [MESH Headings] [Grants] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Received: 09/08/2022] [Revised: 03/23/2023] [Accepted: 04/20/2023] [Indexed: 05/21/2023] Open
Abstract
To facilitate rapid changes in morphology without endangering cell integrity, each cell possesses a substantial amount of cell surface excess (CSE) that can be promptly deployed to cover cell extensions. CSE can be stored in different types of small surface projections such as filopodia, microvilli, and ridges, with rounded bleb-like projections being the most common and rapidly achieved form of storage. We demonstrate that, similar to rounded cells in 2D culture, rounded cells in 3D collagen contain large amounts of CSE and use it to cover developing protrusions. Upon retraction of a protrusion, the CSE this produces is stored over the cell body similar to the CSE produced by cell rounding. We present high-resolution imaging of F-actin and microtubules (MTs) for different cell lines in a 3D environment and demonstrate the correlated changes between CSE and protrusion dynamics. To coordinate CSE storage and release with protrusion formation and motility, we expect cells to have specific mechanisms for regulating CSE, and we hypothesize that MTs play a substantial role in this mechanism by reducing cell surface dynamics and stabilizing CSE. We also suggest that different effects of MT depolymerization on cell motility, such as inhibiting mesenchymal motility and enhancing amoeboid, can be explained by this role of MTs in CSE regulation.
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Affiliation(s)
- Maryna Kapustina
- Department of Cell Biology and Physiology, University of North Carolina at Chapel Hill, Chapel Hill, North Carolina.
| | - Donna Li
- Department of Cell Biology and Physiology, University of North Carolina at Chapel Hill, Chapel Hill, North Carolina
| | - James Zhu
- Department of Cell Biology and Physiology, University of North Carolina at Chapel Hill, Chapel Hill, North Carolina
| | - Brittany Wall
- Department of Cell Biology and Physiology, University of North Carolina at Chapel Hill, Chapel Hill, North Carolina
| | - Violetta Weinreb
- Department of Cell Biology and Physiology, University of North Carolina at Chapel Hill, Chapel Hill, North Carolina
| | - Richard E Cheney
- Department of Cell Biology and Physiology, University of North Carolina at Chapel Hill, Chapel Hill, North Carolina; Lineberger Comprehensive Cancer Center, University of North Carolina at Chapel Hill, Chapel Hill, North Carolina
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7
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Abstract
T cell activation is initiated by the recognition of specific antigenic peptides and subsequently accomplished by complex signaling cascades. These aspects have been extensively studied for decades as pivotal factors in the establishment of adaptive immunity. However, how receptors or signaling molecules are organized in the resting state prior to encountering antigens has received less attention. Recent advancements in super-resolution microscopy techniques have revealed topographically controlled pre-formed organization of key molecules involved in antigen recognition and signal transduction on microvillar projections of T cells before activation and substantial effort has been dedicated to characterizing the topological structure of resting T cells over the past decade. This review will summarize our current understanding of how key surface receptors are pre-organized on the T-cell plasma membrane and discuss the potential role of these receptors, which are preassembled prior to ligand binding in the early activation events of T cells.
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Affiliation(s)
- Yunmin Jung
- Department of Nano-Biomedical Engineering, Advanced Science Institute, Yonsei University, Seoul, Republic of Korea
- Center for Nanomedicine, Institute for Basic Science, Seoul, Republic of Korea
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8
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Baričević Z, Ayar Z, Leitao SM, Mladinic M, Fantner GE, Ban J. Label-Free Long-Term Methods for Live Cell Imaging of Neurons: New Opportunities. BIOSENSORS 2023; 13:404. [PMID: 36979616 PMCID: PMC10046152 DOI: 10.3390/bios13030404] [Citation(s) in RCA: 0] [Impact Index Per Article: 0] [Reference Citation Analysis] [Abstract] [Key Words] [MESH Headings] [Grants] [Track Full Text] [Figures] [Subscribe] [Scholar Register] [Received: 02/18/2023] [Revised: 03/13/2023] [Accepted: 03/15/2023] [Indexed: 06/18/2023]
Abstract
Time-lapse light microscopy combined with in vitro neuronal cultures has provided a significant contribution to the field of Developmental Neuroscience. The establishment of the neuronal polarity, i.e., formation of axons and dendrites, key structures responsible for inter-neuronal signaling, was described in 1988 by Dotti, Sullivan and Banker in a milestone paper that continues to be cited 30 years later. In the following decades, numerous fluorescently labeled tags and dyes were developed for live cell imaging, providing tremendous advancements in terms of resolution, acquisition speed and the ability to track specific cell structures. However, long-term recordings with fluorescence-based approaches remain challenging because of light-induced phototoxicity and/or interference of tags with cell physiology (e.g., perturbed cytoskeletal dynamics) resulting in compromised cell viability leading to cell death. Therefore, a label-free approach remains the most desirable method in long-term imaging of living neurons. In this paper we will focus on label-free high-resolution methods that can be successfully used over a prolonged period. We propose novel tools such as scanning ion conductance microscopy (SICM) or digital holography microscopy (DHM) that could provide new insights into live cell dynamics during neuronal development and regeneration after injury.
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Affiliation(s)
- Zrinko Baričević
- Department of Biotechnology, University of Rijeka, Radmile Matejčić 2, 51000 Rijeka, Croatia; (Z.B.); (M.M.)
| | - Zahra Ayar
- Laboratory for Bio- and Nano-Instrumentation, Institute of Bioengineering, School of Engineering, Swiss Federal Institute of Technology Lausanne (EPFL), 1015 Lausanne, Switzerland; (Z.A.); (S.M.L.)
| | - Samuel M. Leitao
- Laboratory for Bio- and Nano-Instrumentation, Institute of Bioengineering, School of Engineering, Swiss Federal Institute of Technology Lausanne (EPFL), 1015 Lausanne, Switzerland; (Z.A.); (S.M.L.)
| | - Miranda Mladinic
- Department of Biotechnology, University of Rijeka, Radmile Matejčić 2, 51000 Rijeka, Croatia; (Z.B.); (M.M.)
| | - Georg E. Fantner
- Laboratory for Bio- and Nano-Instrumentation, Institute of Bioengineering, School of Engineering, Swiss Federal Institute of Technology Lausanne (EPFL), 1015 Lausanne, Switzerland; (Z.A.); (S.M.L.)
| | - Jelena Ban
- Department of Biotechnology, University of Rijeka, Radmile Matejčić 2, 51000 Rijeka, Croatia; (Z.B.); (M.M.)
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9
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Felipe-López A, Hansmeier N, Danzer C, Hensel M. Manipulation of microvillar proteins during Salmonella enterica invasion results in brush border effacement and actin remodeling. Front Cell Infect Microbiol 2023; 13:1137062. [PMID: 36936760 PMCID: PMC10018140 DOI: 10.3389/fcimb.2023.1137062] [Citation(s) in RCA: 3] [Impact Index Per Article: 1.5] [Reference Citation Analysis] [Abstract] [Key Words] [MESH Headings] [Grants] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Received: 01/03/2023] [Accepted: 02/10/2023] [Indexed: 03/06/2023] Open
Abstract
Enterocyte invasion by the gastrointestinal pathogen Salmonella enterica is accompanied by loss of brush border and massive remodeling of the actin cytoskeleton, leading to microvilli effacement and formation of membrane ruffles. These manipulations are mediated by effector proteins translocated by the Salmonella Pathogenicity Island 1-encoded type III secretion system (SPI1-T3SS). To unravel the mechanisms of microvilli effacement and contribution of SPI1-T3SS effector proteins, the dynamics of host-pathogen interactions was analyzed using live cell imaging (LCI) of polarized epithelial cells (PEC) expressing LifeAct-GFP. PEC were infected with S. enterica wild-type and mutant strains with defined defects in SPI1-T3SS effector proteins, and pharmacological inhibition of actin assembly were applied. We identified that microvilli effacement involves two distinct mechanisms: i) F-actin depolymerization mediated by villin and ii), the consumption of cytoplasmic G-actin by formation of membrane ruffles. By analyzing the contribution of individual SPI1-T3SS effector proteins, we demonstrate that SopE dominantly triggers microvilli effacement and formation of membrane ruffles. Furthermore, SopE via Rac1 indirectly manipulates villin, which culminates in F-actin depolymerization. Collectively, these results indicate that SopE has dual functions during F-actin remodeling in PEC. While SopE-Rac1 triggers F-actin polymerization and ruffle formation, activation of PLCγ and villin by SopE depolymerizes F-actin in PEC. These results demonstrate the key role of SopE in destruction of the intestinal barrier during intestinal infection by Salmonella.
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Affiliation(s)
| | | | - Claudia Danzer
- Mikrobiologisches Institut, Universitätsklinikum Erlangen, Erlangen, Germany
| | - Michael Hensel
- Abt. Mikrobiologie, Universität Osnabrück, Osnabrück, Germany
- *Correspondence: Michael Hensel,
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10
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Wei Y, Wang K, Xia Q, Li B, Liu L. 3D diversiform dynamic process of microvilli in living cells. Biochem Biophys Res Commun 2022; 635:114-119. [DOI: 10.1016/j.bbrc.2022.10.002] [Citation(s) in RCA: 0] [Impact Index Per Article: 0] [Reference Citation Analysis] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Received: 09/09/2022] [Revised: 09/17/2022] [Accepted: 10/01/2022] [Indexed: 11/25/2022]
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11
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Hartmann C, Thüring EM, Greune L, Michels BE, Pajonczyk D, Leußink S, Brinkmann F, Glaesner-Ebnet M, Wardelmann E, Zobel T, Schmidt MA, Janssen KP, Gerke V, Ebnet K. Intestinal brush border formation requires a TMIGD1-based intermicrovillar adhesion complex. Sci Signal 2022; 15:eabm2449. [PMID: 36099341 DOI: 10.1126/scisignal.abm2449] [Citation(s) in RCA: 12] [Impact Index Per Article: 4.0] [Reference Citation Analysis] [Abstract] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Indexed: 11/02/2022]
Abstract
Intestinal epithelial cells absorb nutrients through the brush border, composed of dense arrays of highly ordered microvilli at their apical membranes. A protocadherin-based intermicrovillar adhesion complex localized at microvilli tips mediates microvilli packing and organization. Here, we identified a second adhesion complex localized at the proximal base region of microvilli. This complex contained the immunoglobulin superfamily member TMIGD1, which directly interacted with the microvillar scaffolding proteins EBP50 and E3KARP. Complex formation with EBP50 required the activation of EBP50 by the actin-binding protein ezrin and was enhanced by the dephosphorylation of Ser162 in the PDZ2 domain of EBP50 by the phosphatase PP1α. Binding of the EBP50-ezrin complex to TMIGD1 enhanced the dynamic turnover of EBP50 at microvilli. Enterocyte-specific inactivation of Tmigd1 in mice resulted in microvillar blebbing, loss of intermicrovillar adhesion, and perturbed brush border formation. Thus, we identified a second adhesion complex in microvilli and propose a mechanism that promotes microvillar formation and dynamics.
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Affiliation(s)
- Christian Hartmann
- Institute-associated Research Group "Cell adhesion and cell polarity", ZMBE, University of Münster, D-48149 Münster, Germany.,Institute of Medical Biochemistry, ZMBE, University of Münster, D-48149 Münster, Germany
| | - Eva-Maria Thüring
- Institute-associated Research Group "Cell adhesion and cell polarity", ZMBE, University of Münster, D-48149 Münster, Germany.,Institute of Medical Biochemistry, ZMBE, University of Münster, D-48149 Münster, Germany
| | - Lilo Greune
- Institute of Infectiology, ZMBE, University of Münster, D-48149 Münster, Germany
| | - Birgitta E Michels
- Institute-associated Research Group "Cell adhesion and cell polarity", ZMBE, University of Münster, D-48149 Münster, Germany.,Institute of Medical Biochemistry, ZMBE, University of Münster, D-48149 Münster, Germany
| | - Denise Pajonczyk
- Institute-associated Research Group "Cell adhesion and cell polarity", ZMBE, University of Münster, D-48149 Münster, Germany.,Institute of Medical Biochemistry, ZMBE, University of Münster, D-48149 Münster, Germany
| | - Sophia Leußink
- Institute-associated Research Group "Cell adhesion and cell polarity", ZMBE, University of Münster, D-48149 Münster, Germany.,Institute of Medical Biochemistry, ZMBE, University of Münster, D-48149 Münster, Germany
| | - Frauke Brinkmann
- Institute-associated Research Group "Cell adhesion and cell polarity", ZMBE, University of Münster, D-48149 Münster, Germany.,Institute of Medical Biochemistry, ZMBE, University of Münster, D-48149 Münster, Germany
| | - Mark Glaesner-Ebnet
- Institute-associated Research Group "Cell adhesion and cell polarity", ZMBE, University of Münster, D-48149 Münster, Germany.,Institute of Medical Biochemistry, ZMBE, University of Münster, D-48149 Münster, Germany
| | - Eva Wardelmann
- Gerhard-Domagk-Institute of Pathology, University Hospital Münster, D-48149 Münster, Germany
| | - Thomas Zobel
- Imaging Network Microscopy, University of Münster, D-48149 Münster, Germany
| | - M Alexander Schmidt
- Institute of Infectiology, ZMBE, University of Münster, D-48149 Münster, Germany
| | | | - Volker Gerke
- Institute of Medical Biochemistry, ZMBE, University of Münster, D-48149 Münster, Germany.,Cells-in-Motion Interfaculty Center (CiMIC), University of Münster, D-48419 Münster, Germany
| | - Klaus Ebnet
- Institute-associated Research Group "Cell adhesion and cell polarity", ZMBE, University of Münster, D-48149 Münster, Germany.,Institute of Medical Biochemistry, ZMBE, University of Münster, D-48149 Münster, Germany.,Cells-in-Motion Interfaculty Center (CiMIC), University of Münster, D-48419 Münster, Germany.,Interdisciplinary Center for Clinical Research (IZKF), University of Münster, D-48149 Münster, Germany
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12
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Sun L, Yeo T, Middha E, Gao Y, Lim CT, Watanabe S, Liu B. In Situ Visualization of Dynamic Cellular Effects of Phospholipid Nanoparticles via High-Speed Scanning Ion Conductance Microscopy. SMALL (WEINHEIM AN DER BERGSTRASSE, GERMANY) 2022; 18:e2203285. [PMID: 35946985 DOI: 10.1002/smll.202203285] [Citation(s) in RCA: 11] [Impact Index Per Article: 3.7] [Reference Citation Analysis] [Abstract] [Key Words] [MESH Headings] [Track Full Text] [Subscribe] [Scholar Register] [Received: 05/26/2022] [Revised: 07/02/2022] [Indexed: 06/15/2023]
Abstract
Phospholipid nanoparticles have been actively employed for numerous biomedical applications. A key factor in ensuring effective and safe applications of these nanomaterials is the regulation of their interactions with target cells, which is significantly dependent on an in-depth understanding of the nanoparticle-cell interactions. To date, most studies investigating these nano-bio interactions have been performed under static conditions and may lack crucial real-time information. It is, however, noteworthy that the nanoparticle-cell interactions are highly dynamic. Consequently, to gain a deeper insight into the cellular effects of phospholipid nanoparticles, real-time observation of cellular dynamics after nanoparticle introduction is necessary. Herein, a proof-of-concept in situ visualization of the dynamic cellular effects of sub-100 nm phospholipid nanoparticles using high-speed scanning ion conductance microscopy (HS-SICM) is reported. It is revealed that upon introduction into the cellular environment, within a short timescale of hundreds of seconds, phospholipid nanoparticles can selectively modulate the edge motility and surface roughness of healthy fibroblast and cancerous epithelial cells. Furthermore, the dynamic deformation profiles of these cells can be selectively altered in the presence of phospholipid nanoparticles. This work is anticipated to further shed light on the real-time nanoparticle-cell interactions for improved formulation of phospholipid nanoparticles for numerous bioapplications.
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Affiliation(s)
- Linhao Sun
- Nano Life Science Institute (WPI-NanoLSI), Kanazawa University, Kakuma-machi, Kanazawa, 920-1192, Japan
| | - Trifanny Yeo
- Institute for Health Innovation and Technology, National University of Singapore, MD6, 14 Medical Drive, Singapore, 117599, Singapore
| | - Eshu Middha
- Department of Chemical and Biomolecular Engineering, National University of Singapore, 4 Engineering Drive 4, Singapore, 117585, Singapore
| | - Yuji Gao
- Institute for Health Innovation and Technology, National University of Singapore, MD6, 14 Medical Drive, Singapore, 117599, Singapore
| | - Chwee Teck Lim
- Institute for Health Innovation and Technology, National University of Singapore, MD6, 14 Medical Drive, Singapore, 117599, Singapore
- Department of Biomedical Engineering, National University of Singapore, 9 Engineering Drive 1, Singapore, 117575, Singapore
| | - Shinji Watanabe
- Nano Life Science Institute (WPI-NanoLSI), Kanazawa University, Kakuma-machi, Kanazawa, 920-1192, Japan
| | - Bin Liu
- Department of Chemical and Biomolecular Engineering, National University of Singapore, 4 Engineering Drive 4, Singapore, 117585, Singapore
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13
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Yasunaga T, Wiegel J, Bergen MD, Helmstädter M, Epting D, Paolini A, Çiçek Ö, Radziwill G, Engel C, Brox T, Ronneberger O, Walentek P, Ulbrich MH, Walz G. Microridge-like structures anchor motile cilia. Nat Commun 2022; 13:2056. [PMID: 35440631 PMCID: PMC9018822 DOI: 10.1038/s41467-022-29741-3] [Citation(s) in RCA: 1] [Impact Index Per Article: 0.3] [Reference Citation Analysis] [Abstract] [Key Words] [MESH Headings] [Grants] [Track Full Text] [Download PDF] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Received: 04/01/2021] [Accepted: 03/30/2022] [Indexed: 01/11/2023] Open
Abstract
Several tissues contain cells with multiple motile cilia that generate a fluid or particle flow to support development and organ functions; defective motility causes human disease. Developmental cues orient motile cilia, but how cilia are locked into their final position to maintain a directional flow is not understood. Here we find that the actin cytoskeleton is highly dynamic during early development of multiciliated cells (MCCs). While apical actin bundles become increasingly more static, subapical actin filaments are nucleated from the distal tip of ciliary rootlets. Anchorage of these subapical actin filaments requires the presence of microridge-like structures formed during MCC development, and the activity of Nonmuscle Myosin II. Optogenetic manipulation of Ezrin, a core component of the microridge actin-anchoring complex, or inhibition of Myosin Light Chain Kinase interfere with rootlet anchorage and orientation. These observations identify microridge-like structures as an essential component of basal body rootlet anchoring in MCCs.
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Affiliation(s)
- Takayuki Yasunaga
- Department of Medicine IV, University Freiburg Medical Center, Faculty of Medicine, University of Freiburg, Hugstetter Strasse 55, 79106, Freiburg, Germany
| | - Johannes Wiegel
- Department of Medicine IV, University Freiburg Medical Center, Faculty of Medicine, University of Freiburg, Hugstetter Strasse 55, 79106, Freiburg, Germany
| | - Max D Bergen
- Department of Medicine IV, University Freiburg Medical Center, Faculty of Medicine, University of Freiburg, Hugstetter Strasse 55, 79106, Freiburg, Germany
| | - Martin Helmstädter
- Department of Medicine IV, University Freiburg Medical Center, Faculty of Medicine, University of Freiburg, Hugstetter Strasse 55, 79106, Freiburg, Germany
| | - Daniel Epting
- Department of Medicine IV, University Freiburg Medical Center, Faculty of Medicine, University of Freiburg, Hugstetter Strasse 55, 79106, Freiburg, Germany
| | - Andrea Paolini
- Department of Medicine IV, University Freiburg Medical Center, Faculty of Medicine, University of Freiburg, Hugstetter Strasse 55, 79106, Freiburg, Germany
- Faculty of Biology, University of Freiburg, Schaenzlestrasse 1, 79104, Freiburg, Germany
| | - Özgün Çiçek
- Pattern Recognition and Image Processing, Department of Computer Science, University of Freiburg, Georges-Köhler-Allee 52, 79110, Freiburg, Germany
- BIOSS Centre for Biological Signalling Studies, University of Freiburg, Schänzlestrasse 18, 79104, Freiburg, Germany
| | - Gerald Radziwill
- BIOSS Centre for Biological Signalling Studies, University of Freiburg, Schänzlestrasse 18, 79104, Freiburg, Germany
- CIBSS Centre for Integrative Biological Signalling Studies, University of Freiburg, Schänzlestrasse 18, 79104, Freiburg, Germany
| | - Christina Engel
- Department of Medicine IV, University Freiburg Medical Center, Faculty of Medicine, University of Freiburg, Hugstetter Strasse 55, 79106, Freiburg, Germany
| | - Thomas Brox
- Pattern Recognition and Image Processing, Department of Computer Science, University of Freiburg, Georges-Köhler-Allee 52, 79110, Freiburg, Germany
- BIOSS Centre for Biological Signalling Studies, University of Freiburg, Schänzlestrasse 18, 79104, Freiburg, Germany
- CIBSS Centre for Integrative Biological Signalling Studies, University of Freiburg, Schänzlestrasse 18, 79104, Freiburg, Germany
| | - Olaf Ronneberger
- Pattern Recognition and Image Processing, Department of Computer Science, University of Freiburg, Georges-Köhler-Allee 52, 79110, Freiburg, Germany
- BIOSS Centre for Biological Signalling Studies, University of Freiburg, Schänzlestrasse 18, 79104, Freiburg, Germany
| | - Peter Walentek
- Department of Medicine IV, University Freiburg Medical Center, Faculty of Medicine, University of Freiburg, Hugstetter Strasse 55, 79106, Freiburg, Germany
- CIBSS Centre for Integrative Biological Signalling Studies, University of Freiburg, Schänzlestrasse 18, 79104, Freiburg, Germany
| | - Maximilian H Ulbrich
- Department of Medicine IV, University Freiburg Medical Center, Faculty of Medicine, University of Freiburg, Hugstetter Strasse 55, 79106, Freiburg, Germany
- BIOSS Centre for Biological Signalling Studies, University of Freiburg, Schänzlestrasse 18, 79104, Freiburg, Germany
| | - Gerd Walz
- Department of Medicine IV, University Freiburg Medical Center, Faculty of Medicine, University of Freiburg, Hugstetter Strasse 55, 79106, Freiburg, Germany.
- BIOSS Centre for Biological Signalling Studies, University of Freiburg, Schänzlestrasse 18, 79104, Freiburg, Germany.
- CIBSS Centre for Integrative Biological Signalling Studies, University of Freiburg, Schänzlestrasse 18, 79104, Freiburg, Germany.
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14
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Miyoshi T, Belyantseva IA, Kitajiri SI, Miyajima H, Nishio SY, Usami SI, Kim BJ, Choi BY, Omori K, Shroff H, Friedman TB. Human deafness-associated variants alter the dynamics of key molecules in hair cell stereocilia F-actin cores. Hum Genet 2022; 141:363-382. [PMID: 34232383 PMCID: PMC11351816 DOI: 10.1007/s00439-021-02304-0] [Citation(s) in RCA: 9] [Impact Index Per Article: 3.0] [Reference Citation Analysis] [Abstract] [MESH Headings] [Grants] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Received: 05/05/2021] [Accepted: 06/15/2021] [Indexed: 12/16/2022]
Abstract
Stereocilia protrude up to 100 µm from the apical surface of vertebrate inner ear hair cells and are packed with cross-linked filamentous actin (F-actin). They function as mechanical switches to convert sound vibration into electrochemical neuronal signals transmitted to the brain. Several genes encode molecular components of stereocilia including actin monomers, actin regulatory and bundling proteins, motor proteins and the proteins of the mechanotransduction complex. A stereocilium F-actin core is a dynamic system, which is continuously being remodeled while maintaining an outwardly stable architecture under the regulation of F-actin barbed-end cappers, severing proteins and crosslinkers. The F-actin cores of stereocilia also provide a pathway for motor proteins to transport cargos including components of tip-link densities, scaffolding proteins and actin regulatory proteins. Deficiencies and mutations of stereocilia components that disturb this "dynamic equilibrium" in stereocilia can induce morphological changes and disrupt mechanotransduction causing sensorineural hearing loss, best studied in mouse and zebrafish models. Currently, at least 23 genes, associated with human syndromic and nonsyndromic hearing loss, encode proteins involved in the development and maintenance of stereocilia F-actin cores. However, it is challenging to predict how variants associated with sensorineural hearing loss segregating in families affect protein function. Here, we review the functions of several molecular components of stereocilia F-actin cores and provide new data from our experimental approach to directly evaluate the pathogenicity and functional impact of reported and novel variants of DIAPH1 in autosomal-dominant DFNA1 hearing loss using single-molecule fluorescence microscopy.
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Affiliation(s)
- Takushi Miyoshi
- Laboratory of Molecular Genetics, National Institute on Deafness and Other Communication Disorders, National Institutes of Health, Porter Neuroscience Research Center, Room 1F-143A, Bethesda, MD, 20892, USA.
- Department of Otolaryngology-Head and Neck Surgery, Graduate School of Medicine, Kyoto University, Kyoto, 606-8507, Japan.
| | - Inna A Belyantseva
- Laboratory of Molecular Genetics, National Institute on Deafness and Other Communication Disorders, National Institutes of Health, Porter Neuroscience Research Center, Room 1F-143A, Bethesda, MD, 20892, USA
| | - Shin-Ichiro Kitajiri
- Department of Hearing Implant Sciences, Shinshu University School of Medicine, 390-8621, Matsumoto, Japan
| | - Hiroki Miyajima
- Department of Otolaryngology, Shinshu University School of Medicine, Matsumoto, 390-8621, Japan
- Department of Otolaryngology, Aizawa Hospital, Matsumoto, 390-8510, Japan
| | - Shin-Ya Nishio
- Department of Hearing Implant Sciences, Shinshu University School of Medicine, 390-8621, Matsumoto, Japan
| | - Shin-Ichi Usami
- Department of Hearing Implant Sciences, Shinshu University School of Medicine, 390-8621, Matsumoto, Japan
| | - Bong Jik Kim
- Department of Otolaryngology-Head and Neck Surgery, Chungnam National University College of Medicine, Chungnam National University Sejong Hospital, Sejong, 30099, South Korea
- Brain Research Institute, Chungnam National University College of Medicine, Daejeon, 35015, South Korea
| | - Byung Yoon Choi
- Department of Otorhinolaryngology, Seoul National University Bundang Hospital, Seongnam, 13620, South Korea
| | - Koichi Omori
- Department of Otolaryngology-Head and Neck Surgery, Graduate School of Medicine, Kyoto University, Kyoto, 606-8507, Japan
| | - Hari Shroff
- Laboratory of High Resolution Optical Imaging, National Institute of Biomedical Imaging and Bioengineering, National Institutes of Health, Bethesda, MD, 20892, USA
| | - Thomas B Friedman
- Laboratory of Molecular Genetics, National Institute on Deafness and Other Communication Disorders, National Institutes of Health, Porter Neuroscience Research Center, Room 1F-143A, Bethesda, MD, 20892, USA
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15
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Approach to map nanotopography of cell surface receptors. Commun Biol 2022; 5:218. [PMID: 35264712 PMCID: PMC8907216 DOI: 10.1038/s42003-022-03152-y] [Citation(s) in RCA: 1] [Impact Index Per Article: 0.3] [Reference Citation Analysis] [Abstract] [Track Full Text] [Download PDF] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Received: 08/10/2020] [Accepted: 02/09/2022] [Indexed: 12/18/2022] Open
Abstract
Cells communicate with their environment via surface receptors, but nanoscopic receptor organization with respect to complex cell surface morphology remains unclear. This is mainly due to a lack of accessible, robust and high-resolution methods. Here, we present an approach for mapping the topography of receptors at the cell surface with nanometer precision. The method involves coating glass coverslips with glycine, which preserves the fine membrane morphology while allowing immobilized cells to be positioned close to the optical surface. We developed an advanced and simplified algorithm for the analysis of single-molecule localization data acquired in a biplane detection scheme. These advancements enable direct and quantitative mapping of protein distribution on ruffled plasma membranes with near isotropic 3D nanometer resolution. As demonstrated successfully for CD4 and CD45 receptors, the described workflow is a straightforward quantitative technique to study molecules and their interactions at the complex surface nanomorphology of differentiated metazoan cells. A super-resolution localisation-based method is shown to map receptor topography in immune cells, which allows quantitative study of molecules and their interactions at the complex surface nanomorphology of cells.
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16
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Chen F, He J, Manandhar P, Yang Y, Liu P, Gu N. Gauging surface charge distribution of live cell membrane by ionic current change using scanning ion conductance microscopy. NANOSCALE 2021; 13:19973-19984. [PMID: 34825684 DOI: 10.1039/d1nr05230f] [Citation(s) in RCA: 4] [Impact Index Per Article: 1.0] [Reference Citation Analysis] [Abstract] [MESH Headings] [Track Full Text] [Subscribe] [Scholar Register] [Indexed: 05/23/2023]
Abstract
The distribution of surface charge and potential of cell membrane plays an indispensable role in cellular activities. However, probing surface charge of live cells under physiological conditions, until recently, remains an arduous challenge owing to the lack of effective methods. Scanning ion conductance microscopy (SICM) is an emerging imaging technique for imaging a live cell membrane in its native state. Here, we introduce a simple SICM based imaging technique to effectively map the surface charge contrast distribution of soft substrates including cell membranes by utilizing the higher surface charge sensitivity of the ionic current when the nanopipette tip is close to the substrate with a relatively high current change. This technique was assessed on charged model substrates made of polydimethylsiloxane, and the surface charge sensitivity of ionic current change was supported by finite element method simulations. With this method, we can distinguish the surface charge difference between the cell membrane and the supporting collagen matrix. We also observed the surface charge change induced by the small membrane damage after 1% dimethyl sulfoxide (DMSO) treatment. This new SICM technique provides opportunities to study interfacial and cell membrane processes with high spatial resolution.
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Affiliation(s)
- Feng Chen
- School of Biomedical Engineering and Informatics, Nanjing Medical University, Nanjing 211166, People's Republic of China
- Physics Department, Biomolecular Science Institute, Florida International University, Miami, FL 33199, USA.
| | - Jin He
- Physics Department, Biomolecular Science Institute, Florida International University, Miami, FL 33199, USA.
| | - Prakash Manandhar
- Department of Chemistry and Biochemistry, Florida International University, Miami, FL 33199, USA
| | - Yizi Yang
- School of Biomedical Engineering and Informatics, Nanjing Medical University, Nanjing 211166, People's Republic of China
| | - Peidang Liu
- Jiangsu Key Laboratory for Biomaterials and Devices, School of Biological Science and Medical Engineering, Southeast University, Nanjing 210009, China.
| | - Ning Gu
- School of Biomedical Engineering and Informatics, Nanjing Medical University, Nanjing 211166, People's Republic of China
- Jiangsu Key Laboratory for Biomaterials and Devices, School of Biological Science and Medical Engineering, Southeast University, Nanjing 210009, China.
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17
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Bidaud-Meynard A, Demouchy F, Nicolle O, Pacquelet A, Suman SK, Plancke CN, Robin FB, Michaux G. High-resolution dynamic mapping of the C. elegans intestinal brush border. Development 2021; 148:dev200029. [PMID: 34704594 PMCID: PMC10659032 DOI: 10.1242/dev.200029] [Citation(s) in RCA: 4] [Impact Index Per Article: 1.0] [Reference Citation Analysis] [Abstract] [Key Words] [MESH Headings] [Grants] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Received: 07/26/2021] [Accepted: 10/04/2021] [Indexed: 11/20/2022]
Abstract
The intestinal brush border is made of an array of microvilli that increases the membrane surface area for nutrient processing, absorption and host defense. Studies on mammalian cultured epithelial cells have uncovered some of the molecular players and physical constraints required to establish this apical specialized membrane. However, the building and maintenance of a brush border in vivo has not yet been investigated in detail. Here, we combined super-resolution imaging, transmission electron microscopy and genome editing in the developing nematode Caenorhabditis elegans to build a high-resolution and dynamic localization map of known and new brush border markers. Notably, we show that microvilli components are dynamically enriched at the apical membrane during microvilli outgrowth and maturation, but become highly stable once microvilli are built. This new toolbox will be instrumental for understanding the molecular processes of microvilli growth and maintenance in vivo, as well as the effect of genetic perturbations, notably in the context of disorders affecting brush border integrity.
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Affiliation(s)
- Aurélien Bidaud-Meynard
- Université de Rennes, CNRS, IGDR (Institut de Génétique et Développement de Rennes) - UMR 6290, F-35000 Rennes, France
| | - Flora Demouchy
- Université de Rennes, CNRS, IGDR (Institut de Génétique et Développement de Rennes) - UMR 6290, F-35000 Rennes, France
| | - Ophélie Nicolle
- Université de Rennes, CNRS, IGDR (Institut de Génétique et Développement de Rennes) - UMR 6290, F-35000 Rennes, France
| | - Anne Pacquelet
- Université de Rennes, CNRS, IGDR (Institut de Génétique et Développement de Rennes) - UMR 6290, F-35000 Rennes, France
| | - Shashi Kumar Suman
- Sorbonne Université, Institut Biologie Paris Seine, CNRS UMR7622, Developmental Biology Laboratory, Inserm U1156, F-75005 Paris, France
| | - Camille N Plancke
- Sorbonne Université, Institut Biologie Paris Seine, CNRS UMR7622, Developmental Biology Laboratory, Inserm U1156, F-75005 Paris, France
| | - François B Robin
- Sorbonne Université, Institut Biologie Paris Seine, CNRS UMR7622, Developmental Biology Laboratory, Inserm U1156, F-75005 Paris, France
| | - Grégoire Michaux
- Université de Rennes, CNRS, IGDR (Institut de Génétique et Développement de Rennes) - UMR 6290, F-35000 Rennes, France
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18
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Pleeging R, Ibis F, Fan D, Sasso L, Eral H, Staufer U. Polymer nano manufacturing of a biomimicking surface for kidney stone crystallization studies. MICRO AND NANO ENGINEERING 2021. [DOI: 10.1016/j.mne.2021.100094] [Citation(s) in RCA: 2] [Impact Index Per Article: 0.5] [Reference Citation Analysis] [Track Full Text] [Subscribe] [Scholar Register] [Indexed: 12/13/2022]
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19
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Sommi P, Vitali A, Coniglio S, Callegari D, Barbieri S, Casu A, Falqui A, Vigano’ L, Vigani B, Ferrari F, Anselmi-Tamburini U. Microvilli Adhesion: An Alternative Route for Nanoparticle Cell Internalization. ACS NANO 2021; 15:15803-15814. [PMID: 34585565 PMCID: PMC8552441 DOI: 10.1021/acsnano.1c03151] [Citation(s) in RCA: 11] [Impact Index Per Article: 2.8] [Reference Citation Analysis] [Abstract] [Key Words] [MESH Headings] [Grants] [Track Full Text] [Subscribe] [Scholar Register] [Received: 04/14/2021] [Accepted: 09/24/2021] [Indexed: 05/31/2023]
Abstract
The cellular uptake of nanoparticles (NPs) represents a critical step in nanomedicine and a crucial point for understanding the interaction of nanomaterials with biological systems. No specific mechanism of uptake has been identified so far, as the NPs are generally incorporated by the cells through one of the few well-known endocytotic mechanisms. Here, an alternative internalization route mediated by microvilli adhesion is demonstrated. This microvillus-mediated adhesion (MMA) has been observed using ceria and magnetite NPs with a dimension of <40 nm functionalized with polyacrylic acid but not using NPs with a neutral or positive functionalization. Such an adhesion was not cell specific, as it was demonstrated in three different cell lines. MMA was also reduced by modifications of the microvillus lipid rafts, obtained by depleting cholesterol and altering synthesis of sphingolipids. We found a direct relationship between MAA, cell cycle, and density of microvilli. The evidence suggests that MMA differs from the commonly described uptake mechanisms and might represent an interesting alternative approach for selective NP delivery.
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Affiliation(s)
- Patrizia Sommi
- Human
Physiology Unit, Department of Molecular Medicine, University of Pavia, Via Forlanini 6, 27100 Pavia, Italy
| | - Agostina Vitali
- Department
of Chemistry, University of Pavia, 27100 Pavia, Italy
| | - Stefania Coniglio
- Human
Physiology Unit, Department of Molecular Medicine, University of Pavia, Via Forlanini 6, 27100 Pavia, Italy
| | | | - Sofia Barbieri
- Department
of Physics, University of Pavia, 27100 Pavia, Italy
| | - Alberto Casu
- Biological
and Environmental Sciences and Engineering Division, NABLA Lab, King Abdullah University of Science and Technology
(KAUST), 23955-6900 Thuwal, Saudi Arabia
| | - Andrea Falqui
- Biological
and Environmental Sciences and Engineering Division, NABLA Lab, King Abdullah University of Science and Technology
(KAUST), 23955-6900 Thuwal, Saudi Arabia
| | - Lorenzo Vigano’
- Department
of Chemistry, University of Pavia, 27100 Pavia, Italy
| | - Barbara Vigani
- Department
of Drug Sciences, University of Pavia, 27100 Pavia, Italy
| | - Franca Ferrari
- Department
of Drug Sciences, University of Pavia, 27100 Pavia, Italy
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20
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Abstract
Scanning ion conductance microscopy (SICM) has emerged as a versatile tool for studies of interfaces in biology and materials science with notable utility in biophysical and electrochemical measurements. The heart of the SICM is a nanometer-scale electrolyte filled glass pipette that serves as a scanning probe. In the initial conception, manipulations of ion currents through the tip of the pipette and appropriate positioning hardware provided a route to recording micro- and nanoscopic mapping of the topography of surfaces. Subsequent advances in instrumentation, probe design, and methods significantly increased opportunities for SICM beyond recording topography. Hybridization of SICM with coincident characterization techniques such as optical microscopy and faradaic electrodes have brought SICM to the forefront as a tool for nanoscale chemical measurement for a wide range of applications. Modern approaches to SICM realize an important tool in analytical, bioanalytical, biophysical, and materials measurements, where significant opportunities remain for further exploration. In this review, we chronicle the development of SICM from the perspective of both the development of instrumentation and methods and the breadth of measurements performed.
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Affiliation(s)
- Cheng Zhu
- Department of Chemistry, Indiana University, 800 E. Kirkwood Avenue, Bloomington, Indiana 47405, United States
| | - Kaixiang Huang
- Department of Chemistry, Indiana University, 800 E. Kirkwood Avenue, Bloomington, Indiana 47405, United States
| | - Natasha P Siepser
- Department of Chemistry, Indiana University, 800 E. Kirkwood Avenue, Bloomington, Indiana 47405, United States
| | - Lane A Baker
- Department of Chemistry, Indiana University, 800 E. Kirkwood Avenue, Bloomington, Indiana 47405, United States
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21
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Gaeta IM, Meenderink LM, Postema MM, Cencer CS, Tyska MJ. Direct visualization of epithelial microvilli biogenesis. Curr Biol 2021; 31:2561-2575.e6. [PMID: 33951456 PMCID: PMC8222192 DOI: 10.1016/j.cub.2021.04.012] [Citation(s) in RCA: 38] [Impact Index Per Article: 9.5] [Reference Citation Analysis] [Abstract] [Key Words] [MESH Headings] [Grants] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Received: 10/29/2020] [Revised: 03/12/2021] [Accepted: 04/08/2021] [Indexed: 11/21/2022]
Abstract
Microvilli are actin-bundle-supported surface protrusions that play essential roles in diverse epithelial functions. To develop our understanding of microvilli biogenesis, we used live imaging to directly visualize protrusion growth at early stages of epithelial differentiation. Time-lapse data revealed that specific factors, including epidermal growth factor pathway substrate 8 (EPS8) and insulin-receptor tyrosine kinase substrate (IRTKS) (also known as BAIAP2L1), appear in diffraction-limited puncta at the cell surface and mark future sites of microvillus growth. New core actin bundles elongate from these puncta in parallel with the arrival of ezrin and subsequent plasma membrane encapsulation. In addition to de novo growth, we also observed that new microvilli emerge from pre-existing protrusions. Moreover, we found that nascent microvilli can also collapse, characterized first by loss of membrane wrapping and ezrin enrichment, followed by a sharp decrease in distal tip EPS8 and IRTKS levels, and ultimately disassembly of the core actin bundle itself. These studies are the first to offer a temporally resolved microvillus growth mechanism and highlight factors that participate in this process; they also provide important insights on the growth of apical specializations that will likely apply to diverse epithelial contexts.
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Affiliation(s)
- Isabella M Gaeta
- Department of Cell and Developmental Biology, Vanderbilt University, Nashville, TN 37232, USA
| | - Leslie M Meenderink
- Department of Medicine, Division of Infectious Diseases, Vanderbilt University Medical Center, Nashville, TN 37232, USA; Veterans Affairs Tennessee Valley Health Care System, Nashville, TN 37212, USA
| | - Meagan M Postema
- Department of Cell and Developmental Biology, Vanderbilt University, Nashville, TN 37232, USA
| | - Caroline S Cencer
- Department of Cell and Developmental Biology, Vanderbilt University, Nashville, TN 37232, USA
| | - Matthew J Tyska
- Department of Cell and Developmental Biology, Vanderbilt University, Nashville, TN 37232, USA.
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22
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Taira N, Nashimoto Y, Ino K, Ida H, Imaizumi T, Kumatani A, Takahashi Y, Shiku H. Micropipet-Based Navigation in a Microvascular Model for Imaging Endothelial Cell Topography Using Scanning Ion Conductance Microscopy. Anal Chem 2021; 93:4902-4908. [PMID: 33710857 DOI: 10.1021/acs.analchem.0c05174] [Citation(s) in RCA: 11] [Impact Index Per Article: 2.8] [Reference Citation Analysis] [Abstract] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Indexed: 01/03/2023]
Abstract
Scanning ion conductance microscopy (SICM) has enabled cell surface topography at a high resolution with low invasiveness. However, SICM has not been applied to the observation of cell surfaces in hydrogels, which can serve as scaffolds for three-dimensional cell culture. In this study, we applied SICM for imaging a cell surface in a microvascular lumen reconstructed in a hydrogel. To achieve this goal, we developed a micropipet navigation technique using ionic current to detect the position of a microvascular lumen. Combining this navigation technique with SICM, endothelial cells in a microvascular model and blebs were visualized successfully at the single-cell level. To the best of our knowledge, this is the first report on visualizing cell surfaces in hydrogels using a SICM. This technique will be useful for furthering our understanding of the mechanism of intravascular diseases.
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Affiliation(s)
- Noriko Taira
- Graduate School of Environmental Studies, Tohoku University, Sendai, Miyagi 980-8579, Japan
| | - Yuji Nashimoto
- Graduate School of Environmental Studies, Tohoku University, Sendai, Miyagi 980-8579, Japan.,Graduate School of Engineering, Tohoku University, Sendai, Miyagi 980-8579, Japan.,Frontier Research Institute for Interdisciplinary Sciences (FRIS), Tohoku University, Sendai, Miyagi 980-8578, Japan
| | - Kosuke Ino
- Graduate School of Environmental Studies, Tohoku University, Sendai, Miyagi 980-8579, Japan.,Graduate School of Engineering, Tohoku University, Sendai, Miyagi 980-8579, Japan
| | - Hiroki Ida
- Graduate School of Environmental Studies, Tohoku University, Sendai, Miyagi 980-8579, Japan.,Frontier Research Institute for Interdisciplinary Sciences (FRIS), Tohoku University, Sendai, Miyagi 980-8578, Japan.,WPI-Advanced Institute for Materials Research, Tohoku University, Sendai, Miyagi 980-8577, Japan.,Precursory Research for Embryonic Science and Technology (PRESTO), Science and Technology Agency (JST), Kawaguchi, Saitama 332-0012, Japan
| | - Takuto Imaizumi
- Graduate School of Environmental Studies, Tohoku University, Sendai, Miyagi 980-8579, Japan
| | - Akichika Kumatani
- Graduate School of Environmental Studies, Tohoku University, Sendai, Miyagi 980-8579, Japan.,WPI-Advanced Institute for Materials Research, Tohoku University, Sendai, Miyagi 980-8577, Japan.,WPI-International Center for Materials Nanoarchitectonics, National Institute for Materials Science, Tsukuba, Ibaraki 305-0044, Japan.,Center for Science and Innovation in Spintronics, Tohoku University, Sendai, Miyagi 980-8577, Japan
| | - Yasufumi Takahashi
- Precursory Research for Embryonic Science and Technology (PRESTO), Science and Technology Agency (JST), Kawaguchi, Saitama 332-0012, Japan.,WPI-Nano Life Science Institute, Kanazawa University, Kanazawa, Ishikawa 920-1192, Japan
| | - Hitoshi Shiku
- Graduate School of Environmental Studies, Tohoku University, Sendai, Miyagi 980-8579, Japan.,Graduate School of Engineering, Tohoku University, Sendai, Miyagi 980-8579, Japan
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23
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Cebecauer M. Role of Lipids in Morphogenesis of T-Cell Microvilli. Front Immunol 2021; 12:613591. [PMID: 33790891 PMCID: PMC8006438 DOI: 10.3389/fimmu.2021.613591] [Citation(s) in RCA: 8] [Impact Index Per Article: 2.0] [Reference Citation Analysis] [Abstract] [Key Words] [MESH Headings] [Track Full Text] [Download PDF] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Received: 10/02/2020] [Accepted: 01/13/2021] [Indexed: 11/13/2022] Open
Abstract
T cells communicate with the environment via surface receptors. Cooperation of surface receptors regulates T-cell responses to diverse stimuli. Recently, finger-like membrane protrusions, microvilli, have been demonstrated to play a role in the organization of receptors and, hence, T-cell activation. However, little is known about the morphogenesis of dynamic microvilli, especially in the cells of immune system. In this review, I focus on the potential role of lipids and lipid domains in morphogenesis of microvilli. Discussed is the option that clustering of sphingolipids with phosphoinositides at the plasma membrane results in dimpling (curved) domains. Such domains can attract phosphoinositide-binding proteins and stimulate actin cytoskeleton reorganization. This process triggers cortical actin opening and bundling of actin fibres to support the growing of microvilli. Critical regulators of microvilli morphogenesis in T cells are unknown. At the end, I suggest several candidates with a potential to organize proteins and lipids in these structures.
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Affiliation(s)
- Marek Cebecauer
- Department of Biophysical Chemistry, J. Heyrovsky Institute of Physical Chemistry of the Czech Academy of Sciences (CAS), Prague, Czechia
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24
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Liu X, Wei Y, Li W, Li B, Liu L. Cytoskeleton induced the changes of microvilli and mechanical properties in living cells by atomic force microscopy. J Cell Physiol 2020; 236:3725-3733. [PMID: 33169846 DOI: 10.1002/jcp.30110] [Citation(s) in RCA: 2] [Impact Index Per Article: 0.4] [Reference Citation Analysis] [Abstract] [Key Words] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Received: 08/06/2020] [Revised: 09/08/2020] [Accepted: 10/05/2020] [Indexed: 01/05/2023]
Abstract
The cytoskeleton acts as a scaffold for membrane protrusion, such as microvilli. However, the relationship between the characteristics of microvilli and cytoskeleton remains poorly understood under the physiological state. To investigate the role of the cytoskeleton in regulating microvilli and cellular mechanical properties, atomic force microscopy (AFM) was used to detect the dynamic characteristics of microvillus morphology and elastic modulus of living HeLa cells. First, HeLa and MCF-7 cell lines were stained with Fluor-488-phalloidin and microtubules antibody. Then, the microvilli morphology was analyzed by high-resolution images of AFM in situ. Furthermore, changes in elastic modulus were investigated by the force curve of AFM. Fluorescence microscopy and AFM results revealed that destroyed microfilaments led to a smaller microvilli size, whereas the increase in the aggregation and number of microfilaments led to a larger microvilli size. The destruction and aggregation of microfilaments remarkably affected the mechanical properties of HeLa cells. Microtubule-related drugs induced the change of microtubule, but we failed to note significant differences in microvilli morphology and mechanical properties of cells. In summary, our results unraveled the relationship between microfilaments and the structure of microvilli and Young's modulus in living HeLa cells, which would contribute to the further understanding of the physiological function of the cytoskeleton in vivo.
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Affiliation(s)
- Xueyan Liu
- Key Laboratory of Medicine, School of Laboratory Medicine and Life Sciences, Ministry of Education of China, Wenzhou Medical University, Wenzhou, China
| | - Yuhui Wei
- Division of Physical Biology and Bioimaging Centre, Shanghai Synchrotron Radiation Facility, CAS Key Laboratory of Interfacial Physics and Technology, Chinese Academy of Sciences, Shanghai Institute of Applied Physics, Shanghai, China.,Shanghai Advanced Research Institute, Chinese Academy of Sciences, Shanghai, China
| | - Wei Li
- Key Laboratory of Medicine, School of Laboratory Medicine and Life Sciences, Ministry of Education of China, Wenzhou Medical University, Wenzhou, China.,Zhejiang Provincial Key Laboratory of Medical Genetics, Wenzhou Medical University, Wenzhou, China
| | - Bin Li
- Division of Physical Biology and Bioimaging Centre, Shanghai Synchrotron Radiation Facility, CAS Key Laboratory of Interfacial Physics and Technology, Chinese Academy of Sciences, Shanghai Institute of Applied Physics, Shanghai, China.,Shanghai Advanced Research Institute, Chinese Academy of Sciences, Shanghai, China
| | - Lin Liu
- Key Laboratory of Medicine, School of Laboratory Medicine and Life Sciences, Ministry of Education of China, Wenzhou Medical University, Wenzhou, China.,Division of Physical Biology and Bioimaging Centre, Shanghai Synchrotron Radiation Facility, CAS Key Laboratory of Interfacial Physics and Technology, Chinese Academy of Sciences, Shanghai Institute of Applied Physics, Shanghai, China.,Zhejiang Provincial Key Laboratory of Medical Genetics, Wenzhou Medical University, Wenzhou, China
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25
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van Loon AP, Erofeev IS, Maryshev IV, Goryachev AB, Sagasti A. Cortical contraction drives the 3D patterning of epithelial cell surfaces. J Cell Biol 2020; 219:133677. [PMID: 32003768 PMCID: PMC7054995 DOI: 10.1083/jcb.201904144] [Citation(s) in RCA: 17] [Impact Index Per Article: 3.4] [Reference Citation Analysis] [Abstract] [Track Full Text] [Download PDF] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Received: 04/23/2019] [Revised: 09/16/2019] [Accepted: 12/17/2019] [Indexed: 12/20/2022] Open
Abstract
Cellular protrusions create complex cell surface topographies, but biomechanical mechanisms regulating their formation and arrangement are largely unknown. To study how protrusions form, we focused on the morphogenesis of microridges, elongated actin-based structures that are arranged in maze-like patterns on the apical surfaces of zebrafish skin cells. Microridges form by accreting simple finger-like precursors. Live imaging demonstrated that microridge morphogenesis is linked to apical constriction. A nonmuscle myosin II (NMII) reporter revealed pulsatile contractions of the actomyosin cortex, and inhibiting NMII blocked apical constriction and microridge formation. A biomechanical model suggested that contraction reduces surface tension to permit the fusion of precursors into microridges. Indeed, reducing surface tension with hyperosmolar media promoted microridge formation. In anisotropically stretched cells, microridges formed by precursor fusion along the stretch axis, which computational modeling explained as a consequence of stretch-induced cortical flow. Collectively, our results demonstrate how contraction within the 2D plane of the cortex can pattern 3D cell surfaces.
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Affiliation(s)
- Aaron P van Loon
- Department of Molecular, Cell and Developmental Biology and Molecular Biology Institute, University of California, Los Angeles, Los Angeles, CA
| | - Ivan S Erofeev
- Centre for Synthetic and Systems Biology, School of Biological Sciences, University of Edinburgh, Edinburgh, UK
| | - Ivan V Maryshev
- Centre for Synthetic and Systems Biology, School of Biological Sciences, University of Edinburgh, Edinburgh, UK
| | - Andrew B Goryachev
- Centre for Synthetic and Systems Biology, School of Biological Sciences, University of Edinburgh, Edinburgh, UK
| | - Alvaro Sagasti
- Department of Molecular, Cell and Developmental Biology and Molecular Biology Institute, University of California, Los Angeles, Los Angeles, CA
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26
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Orbach R, Su X. Surfing on Membrane Waves: Microvilli, Curved Membranes, and Immune Signaling. Front Immunol 2020; 11:2187. [PMID: 33013920 PMCID: PMC7516127 DOI: 10.3389/fimmu.2020.02187] [Citation(s) in RCA: 34] [Impact Index Per Article: 6.8] [Reference Citation Analysis] [Abstract] [Key Words] [MESH Headings] [Track Full Text] [Download PDF] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Received: 05/30/2020] [Accepted: 08/11/2020] [Indexed: 01/22/2023] Open
Abstract
Microvilli are finger-like membrane protrusions, supported by the actin cytoskeleton, and found on almost all cell types. A growing body of evidence suggests that the dynamic lymphocyte microvilli, with their highly curved membranes, play an important role in signal transduction leading to immune responses. Nevertheless, challenges in modulating local membrane curvature and monitoring the high dynamicity of microvilli hampered the investigation of the curvature-generation mechanism and its functional consequences in signaling. These technical barriers have been partially overcome by recent advancements in adapted super-resolution microscopy. Here, we review the up-to-date progress in understanding the mechanisms and functional consequences of microvillus formation in T cell signaling. We discuss how the deformation of local membranes could potentially affect the organization of signaling proteins and their biochemical activities. We propose that curved membranes, together with the underlying cytoskeleton, shape microvilli into a unique compartment that sense and process signals leading to lymphocyte activation.
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Affiliation(s)
- Ron Orbach
- Department of Cell Biology, Yale School of Medicine, New Haven, CT, United States
| | - Xiaolei Su
- Department of Cell Biology, Yale School of Medicine, New Haven, CT, United States
- Yale Cancer Center, Yale University, New Haven, CT, United States
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27
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Bednarska J, Pelchen-Matthews A, Novak P, Burden JJ, Summers PA, Kuimova MK, Korchev Y, Marsh M, Shevchuk A. Rapid formation of human immunodeficiency virus-like particles. Proc Natl Acad Sci U S A 2020; 117:21637-21646. [PMID: 32817566 PMCID: PMC7474690 DOI: 10.1073/pnas.2008156117] [Citation(s) in RCA: 17] [Impact Index Per Article: 3.4] [Reference Citation Analysis] [Abstract] [Key Words] [MESH Headings] [Grants] [Track Full Text] [Download PDF] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Indexed: 12/12/2022] Open
Abstract
Understanding the molecular mechanisms involved in the assembly of viruses is essential for discerning how viruses transmit from cell to cell and host to host. Although molecular aspects of assembly have been studied for many viruses, we still have little information about these events in real time. Enveloped viruses such as HIV that assemble at, and bud from, the plasma membrane have been studied in some detail using live cell fluorescence imaging techniques; however, these approaches provide little information about the real-time morphological changes that take place as viral components come together to form individual virus particles. Here we used correlative scanning ion conductance microscopy and fluorescence confocal microscopy to measure the topological changes, together with the recruitment of fluorescently labeled viral proteins such as Gag and Vpr, during the assembly and release of individual HIV virus-like particles (VLPs) from the top, nonadherent surfaces of living cells. We show that 1) labeling of viral proteins with green fluorescent protein affects particle formation, 2) the kinetics of particle assembly on different plasma membrane domains can vary, possibly as a consequence of differences in membrane biophysical properties, and 3) VLPs budding from the top, unimpeded surface of cells can reach full size in 20 s and disappear from the budding site in 0.5 to 3 min from the moment curvature is initially detected, significantly faster than has been previously reported.
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Affiliation(s)
- Joanna Bednarska
- Department of Medicine, Imperial College London, W12 0NN London, United Kingdom
| | - Annegret Pelchen-Matthews
- Medical Research Council Laboratory for Molecular Cell Biology, University College London, WC1E 6BT London, United Kingdom
| | - Pavel Novak
- Department of Medicine, Imperial College London, W12 0NN London, United Kingdom
- Functional Low-Dimensional Structures Laboratory, National University of Science and Technology "MISIS", 119991 Moscow, Russian Federation
| | - Jemima J Burden
- Medical Research Council Laboratory for Molecular Cell Biology, University College London, WC1E 6BT London, United Kingdom
| | - Peter A Summers
- Molecular Sciences Research Hub, Department of Chemistry, Imperial College London, W12 0BZ London, United Kingdom
| | - Marina K Kuimova
- Molecular Sciences Research Hub, Department of Chemistry, Imperial College London, W12 0BZ London, United Kingdom
| | - Yuri Korchev
- Department of Medicine, Imperial College London, W12 0NN London, United Kingdom
- Nano Life Science Institute, Kanazawa University, 920-1192 Kanazawa, Japan
| | - Mark Marsh
- Medical Research Council Laboratory for Molecular Cell Biology, University College London, WC1E 6BT London, United Kingdom;
| | - Andrew Shevchuk
- Department of Medicine, Imperial College London, W12 0NN London, United Kingdom;
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28
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Gesper A, Wennmalm S, Hagemann P, Eriksson SG, Happel P, Parmryd I. Variations in Plasma Membrane Topography Can Explain Heterogenous Diffusion Coefficients Obtained by Fluorescence Correlation Spectroscopy. Front Cell Dev Biol 2020; 8:767. [PMID: 32903922 PMCID: PMC7443568 DOI: 10.3389/fcell.2020.00767] [Citation(s) in RCA: 14] [Impact Index Per Article: 2.8] [Reference Citation Analysis] [Abstract] [Key Words] [Track Full Text] [Download PDF] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Received: 04/30/2020] [Accepted: 07/21/2020] [Indexed: 01/18/2023] Open
Abstract
Fluorescence correlation spectroscopy (FCS) is frequently used to study diffusion in cell membranes, primarily the plasma membrane. The diffusion coefficients reported in the plasma membrane of the same cell type and even within single cells typically display a large spread. We have investigated whether this spread can be explained by variations in membrane topography throughout the cell surface, that changes the amount of membrane in the FCS focal volume at different locations. Using FCS, we found that diffusion of the membrane dye DiI in the apical plasma membrane was consistently faster above the nucleus than above the cytoplasm. Using live cell scanning ion conductance microscopy (SICM) to obtain a topography map of the cell surface, we demonstrate that cell surface roughness is unevenly distributed with the plasma membrane above the nucleus being the smoothest, suggesting that the difference in diffusion observed in FCS is related to membrane topography. FCS modeled on simulated diffusion in cell surfaces obtained by SICM was consistent with the FCS data from live cells and demonstrated that topography variations can cause the appearance of anomalous diffusion in FCS measurements. Furthermore, we found that variations in the amount of the membrane marker DiD, a proxy for the membrane, but not the transmembrane protein TCRζ or the lipid-anchored protein Lck, in the FCS focal volume were related to variations in diffusion times at different positions in the plasma membrane. This relationship was seen at different positions both at the apical cell and basal cell sides. We conclude that it is crucial to consider variations in topography in the interpretation of FCS results from membranes.
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Affiliation(s)
| | - Stefan Wennmalm
- SciLifeLab, Royal Institute of Technology, Stockholm, Sweden
| | | | | | | | - Ingela Parmryd
- Institute of Biomedicine, University of Gothenburg, Gothenburg, Sweden
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29
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Sviben S, Spaeker O, Bennet M, Albéric M, Dirks JH, Moussian B, Fratzl P, Bertinetti L, Politi Y. Epidermal Cell Surface Structure and Chitin-Protein Co-assembly Determine Fiber Architecture in the Locust Cuticle. ACS APPLIED MATERIALS & INTERFACES 2020; 12:25581-25590. [PMID: 32343541 PMCID: PMC7304823 DOI: 10.1021/acsami.0c04572] [Citation(s) in RCA: 17] [Impact Index Per Article: 3.4] [Reference Citation Analysis] [Abstract] [Key Words] [MESH Headings] [Track Full Text] [Subscribe] [Scholar Register] [Indexed: 05/16/2023]
Abstract
The geometrical similarity of helicoidal fiber arrangement in many biological fibrous extracellular matrices, such as bone, plant cell wall, or arthropod cuticle, to that of cholesteric liquid mesophases has led to the hypothesis that they may form passively through a mesophase precursor rather than by direct cellular control. In search of direct evidence to support or refute this hypothesis, here, we studied the process of cuticle formation in the tibia of the migratory locust, Locusta migratoria, where daily growth layers arise by the deposition of fiber arrangements alternating between unidirectional and helicoidal structures. Using focused ion beam/scanning electron microscopy (FIB/SEM) volume imaging and scanning X-ray scattering, we show that the epidermal cells determine an initial fiber orientation, from which the final architecture emerges by the self-organized co-assembly of chitin and proteins. Fiber orientation in the locust cuticle is therefore determined by both active and passive processes.
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Affiliation(s)
- Sanja Sviben
- Department
of Biomaterials, Max Planck Institute of
Colloids and Interfaces, 14476 Potsdam, Germany
| | - Oliver Spaeker
- Department
of Biomaterials, Max Planck Institute of
Colloids and Interfaces, 14476 Potsdam, Germany
| | - Mathieu Bennet
- Department
of Biomaterials, Max Planck Institute of
Colloids and Interfaces, 14476 Potsdam, Germany
| | - Marie Albéric
- Department
of Biomaterials, Max Planck Institute of
Colloids and Interfaces, 14476 Potsdam, Germany
- Laboratoire
Chimie de la Matière Condensée de Paris, Sorbonne Université, UMR CNRS 7574, 75005 Paris, France
| | - Jan-Henning Dirks
- Max
Planck Institute for Intelligent Systems, 70569 Stuttgart, Germany
- Biomimetics-Innovation-Centre, Hochschule Bremen—City University of Applied
Sciences, 28199 Bremen, Germany
| | - Bernard Moussian
- Institute
of Biology Valrose, Université Côte
d’Azur, CNRS, Inserm, Parc Valrose, 06108 Nice Cedex 2, France
| | - Peter Fratzl
- Department
of Biomaterials, Max Planck Institute of
Colloids and Interfaces, 14476 Potsdam, Germany
| | - Luca Bertinetti
- Department
of Biomaterials, Max Planck Institute of
Colloids and Interfaces, 14476 Potsdam, Germany
| | - Yael Politi
- Department
of Biomaterials, Max Planck Institute of
Colloids and Interfaces, 14476 Potsdam, Germany
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30
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Myosin-XVa Controls Both Staircase Architecture and Diameter Gradation of Stereocilia Rows in the Auditory Hair Cell Bundles. J Assoc Res Otolaryngol 2020; 21:121-135. [PMID: 32152769 DOI: 10.1007/s10162-020-00745-4] [Citation(s) in RCA: 12] [Impact Index Per Article: 2.4] [Reference Citation Analysis] [Abstract] [Key Words] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Received: 08/29/2019] [Accepted: 02/04/2020] [Indexed: 02/08/2023] Open
Abstract
Mammalian hair cells develop their mechanosensory bundles through consecutive phases of stereocilia elongation, thickening, and retraction of supernumerary stereocilia. Many molecules involved in stereocilia elongation have been identified, including myosin-XVa. Significantly less is known about molecular mechanisms of stereocilia thickening and retraction. Here, we used scanning electron microscopy (SEM) to quantify postnatal changes in number and diameters of the auditory hair cell stereocilia in shaker-2 mice (Myo15sh2) that lack both "long" and "short" isoforms of myosin-XVa, and in mice lacking only the "long" myosin-XVa isoform (Myo15∆N). Previously, we observed large mechanotransduction current in young postnatal inner (IHC) and outer (OHC) hair cells of both these strains. Stereocilia counts showed nearly identical developmental retraction of supernumerary stereocilia in control heterozygous, Myo15sh2/sh2, and Myo15∆N/∆N mice, suggesting that this retraction is largely unaffected by myosin-XVa deficiency. However, myosin-XVa deficiency does affect stereocilia diameters. In control, the first (tallest) and second row stereocilia grow in diameter simultaneously. However, the third row stereocilia in IHCs grow only until postnatal day 1-2 and then become thinner. In OHCs, they also grow slower than taller stereocilia, forming a stereocilia diameter gradation within a hair bundle. The sh2 mutation disrupts this gradation and makes all stereocilia nearly identical in thickness in both IHCs and OHCs, with only subtle residual diameter differences. All Myo15sh2/sh2 stereocilia grow postnatally including the third row, which is not a part of normal development. Serial sections with focused ion beam (FIB)-SEM confirmed that diameter changes of Myo15sh2/sh2 IHC and OHC stereocilia resulted from corresponding changes of their actin cores. In contrast to Myo15sh2/sh2, Myo15∆N/∆N hair cells develop prominent stereocilia diameter gradation. Thus, besides building the staircase, the short isoform of myosin-XVa is essential for controlling the diameter of the third row stereocilia and formation of the stereocilia diameter gradation in a hair bundle.
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31
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Jin R, Huang Y, Cheng L, Lu H, Jiang D, Chen HY. In situ observation of heterogeneous charge distribution at the electrode unraveling the mechanism of electric field-enhanced electrochemical activity. Chem Sci 2020. [DOI: 10.1039/d0sc00223b] [Citation(s) in RCA: 5] [Impact Index Per Article: 1.0] [Reference Citation Analysis] [Abstract] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Indexed: 11/21/2022] Open
Abstract
In situ observation of heterogeneous charge distribution at the Pt–graphite surface in the hydrogen evolution reaction is realized using scanning ion conductive microscopy.
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Affiliation(s)
- Rong Jin
- State Key Laboratory of Analytical Chemistry for Life Science
- School of Chemistry and Chemical Engineering
- Nanjing University
- Nanjing
- P. R. China
| | - Yuchen Huang
- State Key Laboratory of Analytical Chemistry for Life Science
- School of Chemistry and Chemical Engineering
- Nanjing University
- Nanjing
- P. R. China
| | - Lei Cheng
- School of Mechanical Engineering
- Xi'an Jiaotong University
- Xi'an
- P. R. China
| | - Hongyan Lu
- State Key Laboratory of Analytical Chemistry for Life Science
- School of Chemistry and Chemical Engineering
- Nanjing University
- Nanjing
- P. R. China
| | - Dechen Jiang
- State Key Laboratory of Analytical Chemistry for Life Science
- School of Chemistry and Chemical Engineering
- Nanjing University
- Nanjing
- P. R. China
| | - Hong-Yuan Chen
- State Key Laboratory of Analytical Chemistry for Life Science
- School of Chemistry and Chemical Engineering
- Nanjing University
- Nanjing
- P. R. China
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32
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Watanabe S, Kitazawa S, Sun L, Kodera N, Ando T. Development of high-speed ion conductance microscopy. THE REVIEW OF SCIENTIFIC INSTRUMENTS 2019; 90:123704. [PMID: 31893861 DOI: 10.1063/1.5118360] [Citation(s) in RCA: 15] [Impact Index Per Article: 2.5] [Reference Citation Analysis] [Abstract] [Track Full Text] [Subscribe] [Scholar Register] [Indexed: 05/17/2023]
Abstract
Scanning ion conductance microscopy (SICM) can image the surface topography of specimens in ionic solutions without mechanical probe-sample contact. This unique capability is advantageous for imaging fragile biological samples but its highest possible imaging rate is far lower than the level desired in biological studies. Here, we present the development of high-speed SICM. The fast imaging capability is attained by a fast Z-scanner with active vibration control and pipette probes with enhanced ion conductance. By the former, the delay of probe Z-positioning is minimized to sub-10 µs, while its maximum stroke is secured at 6 μm. The enhanced ion conductance lowers a noise floor in ion current detection, increasing the detection bandwidth up to 100 kHz. Thus, temporal resolution 100-fold higher than that of conventional systems is achieved, together with spatial resolution around 20 nm.
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Affiliation(s)
- Shinji Watanabe
- WPI Nano Life Science Institute (WPI-NanoLSI), Kanazawa University, Kakuma-machi, Kanazawa 920-1192, Japan
| | - Satoko Kitazawa
- Department of Physics, Institute of Science and Engineering, Kanazawa University, Kakuma-machi, Kanazawa 920-1192, Japan
| | - Linhao Sun
- WPI Nano Life Science Institute (WPI-NanoLSI), Kanazawa University, Kakuma-machi, Kanazawa 920-1192, Japan
| | - Noriyuki Kodera
- WPI Nano Life Science Institute (WPI-NanoLSI), Kanazawa University, Kakuma-machi, Kanazawa 920-1192, Japan
| | - Toshio Ando
- WPI Nano Life Science Institute (WPI-NanoLSI), Kanazawa University, Kakuma-machi, Kanazawa 920-1192, Japan
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33
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Microridges are apical epithelial projections formed of F-actin networks that organize the glycan layer. Sci Rep 2019; 9:12191. [PMID: 31434932 PMCID: PMC6704121 DOI: 10.1038/s41598-019-48400-0] [Citation(s) in RCA: 24] [Impact Index Per Article: 4.0] [Reference Citation Analysis] [Abstract] [Track Full Text] [Download PDF] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Received: 11/12/2018] [Accepted: 07/29/2019] [Indexed: 11/16/2022] Open
Abstract
Apical projections are integral functional units of epithelial cells. Microvilli and stereocilia are cylindrical apical projections that are formed of bundled actin. Microridges on the other hand, extend laterally, forming labyrinthine patterns on surfaces of various kinds of squamous epithelial cells. So far, the structural organization and functions of microridges have remained elusive. We have analyzed microridges on zebrafish epidermal cells using confocal and electron microscopy methods including electron tomography, to show that microridges are formed of F-actin networks and require the function of the Arp2/3 complex for their maintenance. During development, microridges begin as F-actin punctae showing signatures of branching and requiring an active Arp2/3 complex. Using inhibitors of actin polymerization and the Arp2/3 complex, we show that microridges organize the surface glycan layer. Our analyses have unraveled the F-actin organization supporting the most abundant and evolutionarily conserved apical projection, which functions in glycan organization.
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34
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Simeonov S, Schäffer TE. High-speed scanning ion conductance microscopy for sub-second topography imaging of live cells. NANOSCALE 2019; 11:8579-8587. [PMID: 30994121 DOI: 10.1039/c8nr10162k] [Citation(s) in RCA: 26] [Impact Index Per Article: 4.3] [Reference Citation Analysis] [Abstract] [MESH Headings] [Track Full Text] [Subscribe] [Scholar Register] [Indexed: 05/17/2023]
Abstract
Scanning ion conductance microscopy (SICM) is an emerging tool for non-invasive and high-resolution topography imaging of live cells. However, the imaging speed of conventional SICM setups is slow, requiring several seconds or even minutes per image, thereby making it difficult to study cellular dynamics. Here, we describe a high-speed SICM (HS-SICM) setup for topography imaging in the hopping mode with a pixel rate of 11.0 kHz, which is 15 times faster than what was reported before. In combination with a "turn step" procedure for rapid pipette retraction, we image the ultra-fast morphodynamics of live human platelets, A6 cells, and U2OS cells at a rate as fast as 0.6 s per frame. The results show that HS-SICM provides a useful platform for investigating the dynamics of cell morphology on a sub-second timescale.
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Affiliation(s)
- Stefan Simeonov
- Institute of Applied Physics, University of Tübingen, Auf der Morgenstelle 10, 72076 Tübingen, Germany.
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35
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Rheinlaender J, Schäffer TE. Mapping the creep compliance of living cells with scanning ion conductance microscopy reveals a subcellular correlation between stiffness and fluidity. NANOSCALE 2019; 11:6982-6989. [PMID: 30916074 DOI: 10.1039/c8nr09428d] [Citation(s) in RCA: 11] [Impact Index Per Article: 1.8] [Reference Citation Analysis] [Abstract] [MESH Headings] [Track Full Text] [Subscribe] [Scholar Register] [Indexed: 06/09/2023]
Abstract
Living cells exhibit complex material properties, which play a crucial role in many aspects of cell function in health and disease, including migration, proliferation, differentiation, and apoptosis. Various techniques exist to probe the viscoelastic material properties of living cells and a frequent observation is a cell-to-cell correlation between average stiffness and fluidity in populations of cells. However, the origin of this correlation is still under discussion. Here, we introduce an imaging technique based on the scanning ion conductance microscope (SICM) to measure the creep compliance of soft samples, which allowed us to generate images of viscoelastic material properties of living cells with high spatial and temporal resolution. We observe a strong subcellular correlation between the local stiffness and fluidity across the individual living cell: stiff regions exhibit lower fluidity while soft regions exhibit higher fluidity. We find that this subcellular correlation is identical to the previously observed cell-to-cell correlation. The subcellular correlation reversibly vanishes after drug-induced disruption of the cytoskeleton, indicating that the subcellular correlation is a property of the intact cytoskeleton of the living cell.
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Affiliation(s)
- Johannes Rheinlaender
- Institute of Applied Physics, University of Tübingen, Auf der Morgenstelle 10, 72076 Tübingen, Germany.
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36
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Depasquale JA. Actin Microridges. Anat Rec (Hoboken) 2018; 301:2037-2050. [DOI: 10.1002/ar.23965] [Citation(s) in RCA: 19] [Impact Index Per Article: 2.7] [Reference Citation Analysis] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Received: 02/13/2018] [Revised: 05/03/2018] [Accepted: 05/14/2018] [Indexed: 12/21/2022]
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37
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DePasquale JA. Comparison of microridges in juvenile and adult sunfish,
Lepomis gibbosus. ACTA ZOOL-STOCKHOLM 2018. [DOI: 10.1111/azo.12281] [Citation(s) in RCA: 1] [Impact Index Per Article: 0.1] [Reference Citation Analysis] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Indexed: 11/30/2022]
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38
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Cebecauer M, Amaro M, Jurkiewicz P, Sarmento MJ, Šachl R, Cwiklik L, Hof M. Membrane Lipid Nanodomains. Chem Rev 2018; 118:11259-11297. [PMID: 30362705 DOI: 10.1021/acs.chemrev.8b00322] [Citation(s) in RCA: 146] [Impact Index Per Article: 20.9] [Reference Citation Analysis] [Abstract] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Indexed: 12/15/2022]
Abstract
Lipid membranes can spontaneously organize their components into domains of different sizes and properties. The organization of membrane lipids into nanodomains might potentially play a role in vital functions of cells and organisms. Model membranes represent attractive systems to study lipid nanodomains, which cannot be directly addressed in living cells with the currently available methods. This review summarizes the knowledge on lipid nanodomains in model membranes and exposes how their specific character contrasts with large-scale phase separation. The overview on lipid nanodomains in membranes composed of diverse lipids (e.g., zwitterionic and anionic glycerophospholipids, ceramides, glycosphingolipids) and cholesterol aims to evidence the impact of chemical, electrostatic, and geometric properties of lipids on nanodomain formation. Furthermore, the effects of curvature, asymmetry, and ions on membrane nanodomains are shown to be highly relevant aspects that may also modulate lipid nanodomains in cellular membranes. Potential mechanisms responsible for the formation and dynamics of nanodomains are discussed with support from available theories and computational studies. A brief description of current fluorescence techniques and analytical tools that enabled progress in lipid nanodomain studies is also included. Further directions are proposed to successfully extend this research to cells.
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Affiliation(s)
- Marek Cebecauer
- J. Heyrovský Institute of Physical Chemistry of the Czech Academy of Sciences , Dolejškova 3 , 18223 Prague 8 , Czech Republic
| | - Mariana Amaro
- J. Heyrovský Institute of Physical Chemistry of the Czech Academy of Sciences , Dolejškova 3 , 18223 Prague 8 , Czech Republic
| | - Piotr Jurkiewicz
- J. Heyrovský Institute of Physical Chemistry of the Czech Academy of Sciences , Dolejškova 3 , 18223 Prague 8 , Czech Republic
| | - Maria João Sarmento
- J. Heyrovský Institute of Physical Chemistry of the Czech Academy of Sciences , Dolejškova 3 , 18223 Prague 8 , Czech Republic
| | - Radek Šachl
- J. Heyrovský Institute of Physical Chemistry of the Czech Academy of Sciences , Dolejškova 3 , 18223 Prague 8 , Czech Republic
| | - Lukasz Cwiklik
- J. Heyrovský Institute of Physical Chemistry of the Czech Academy of Sciences , Dolejškova 3 , 18223 Prague 8 , Czech Republic
| | - Martin Hof
- J. Heyrovský Institute of Physical Chemistry of the Czech Academy of Sciences , Dolejškova 3 , 18223 Prague 8 , Czech Republic
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Pelaseyed T, Bretscher A. Regulation of actin-based apical structures on epithelial cells. J Cell Sci 2018; 131:131/20/jcs221853. [PMID: 30333133 DOI: 10.1242/jcs.221853] [Citation(s) in RCA: 65] [Impact Index Per Article: 9.3] [Reference Citation Analysis] [Abstract] [Key Words] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Indexed: 01/03/2023] Open
Abstract
Cells of transporting epithelia are characterized by the presence of abundant F-actin-based microvilli on their apical surfaces. Likewise, auditory hair cells have highly reproducible rows of apical stereocilia (giant microvilli) that convert mechanical sound into an electrical signal. Analysis of mutations in deaf patients has highlighted the critical components of tip links between stereocilia, and related structures that contribute to the organization of microvilli on epithelial cells have been found. Ezrin/radixin/moesin (ERM) proteins, which are activated by phosphorylation, provide a critical link between the plasma membrane and underlying actin cytoskeleton in surface structures. Here, we outline recent insights into how microvilli and stereocilia are built, and the roles of tip links. Furthermore, we highlight how ezrin is locally regulated by phosphorylation, and that this is necessary to maintain polarity. Localized phosphorylation is achieved through an intricate coincidence detection mechanism that requires the membrane lipid phosphatidylinositol 4,5-bisphosphate [PI(4,5)P2] and the apically localized ezrin kinase, lymphocyte-oriented kinase (LOK, also known as STK10) or Ste20-like kinase (SLK). We also discuss how ezrin-binding scaffolding proteins regulate microvilli and how, despite these significant advances, it remains to be discovered how the cell polarity program ultimately interfaces with these processes.
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Affiliation(s)
- Thaher Pelaseyed
- Institute of Biomedicine, Department of Medical Biochemistry and Cell Biology, University of Gothenburg, SE-405 30 Gothenburg, Sweden
| | - Anthony Bretscher
- Weill Institute for Cell and Molecular Biology, Department of Molecular Biology and Genetics, Cornell University, Ithaca, NY 14853, USA
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40
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Affiliation(s)
- Kosuke Ino
- Graduate School of Engineering; Tohoku University; 6-6-11 Aramaki-aza Aoba, Aoba-ku Sendai 980-8579 Japan
| | - Yuji Nashimoto
- Graduate School of Engineering; Tohoku University; 6-6-11 Aramaki-aza Aoba, Aoba-ku Sendai 980-8579 Japan
- Frontier Research Institute for Interdisciplinary Sciences; Tohoku University; 6-3 Aramaki-aza Aoba, Aoba-ku Sendai 980-8578 Japan
| | - Noriko Taira
- Graduate School of Engineering; Tohoku University; 6-6-11 Aramaki-aza Aoba, Aoba-ku Sendai 980-8579 Japan
| | - Javier Ramon Azcon
- Institute for Bioengineering of Catalonia (IBEC); The Barcelona Institute of Science and Technology; Baldiri Reixac 10-12 08028 Barcelona Spain
| | - Hitoshi Shiku
- Graduate School of Engineering; Tohoku University; 6-6-11 Aramaki-aza Aoba, Aoba-ku Sendai 980-8579 Japan
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41
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Li Y, Jia S, Liu H, Tateya T, Guo W, Yang S, Beisel KW, He DZZ. Characterization of Hair Cell-Like Cells Converted From Supporting Cells After Notch Inhibition in Cultures of the Organ of Corti From Neonatal Gerbils. Front Cell Neurosci 2018; 12:73. [PMID: 29662441 PMCID: PMC5890164 DOI: 10.3389/fncel.2018.00073] [Citation(s) in RCA: 10] [Impact Index Per Article: 1.4] [Reference Citation Analysis] [Abstract] [Key Words] [Track Full Text] [Download PDF] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Received: 09/07/2017] [Accepted: 03/02/2018] [Indexed: 12/11/2022] Open
Abstract
The senses of hearing and balance depend upon hair cells, the sensory receptors of the inner ear. Hair cells transduce mechanical stimuli into electrical activity. Loss of hair cells as a result of aging or exposure to noise and ototoxic drugs is the major cause of noncongenital hearing and balance deficits. In the ear of non-mammals, lost hair cells can spontaneously be replaced by production of new hair cells from conversion of supporting cells. Although supporting cells in adult mammals have lost that capability, neonatal supporting cells are able to convert to hair cells after inhibition of Notch signaling. We questioned whether Notch inhibition is sufficient to convert supporting cells to functional hair cells using electrophysiology and electron microscopy. We showed that pharmacological inhibition of the canonical Notch pathway in the cultured organ of Corti prepared from neonatal gerbils induced stereocilia formation in supporting cells (defined as hair cell-like cells or HCLCs) and supernumerary stereocilia in hair cells. The newly emerged stereocilia bundles of HCLCs were functional, i.e., able to respond to mechanical stimulation with mechanotransduction (MET) current. Transmission electron microscopy (TEM) showed that HCLCs converted from pillar cells maintained the pillar cell shape and that subsurface cisternae, normally observed underneath the cytoskeleton in outer hair cells (OHCs), was not present in Deiters’ cells-derived HCLCs. Voltage-clamp recordings showed that whole-cell currents from Deiters’ cells-derived HCLCs retained the same kinetics and magnitude seen in normal Deiters’ cells and that nonlinear capacitance (NLC), an electrical hallmark of OHC electromotility, was not detected from any HCLCs measured. Taken together, these results suggest that while Notch inhibition is sufficient for promoting stereocilia bundle formation, it is insufficient to convert neonatal supporting cells to mature hair cells. The fact that Notch inhibition led to stereocilia formation in supporting cells and supernumerary stereocilia in existing hair cells appears to suggest that Notch signaling may regulate stereocilia formation and stability during development.
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Affiliation(s)
- Yi Li
- Department of Otorhinolaryngology, Beijing Tongren Hospital, Beijing Capital Medical University, Beijing, China.,Department of Biomedical Sciences, Creighton University School of Medicine, Omaha, NE, United States
| | - Shuping Jia
- Department of Biomedical Sciences, Creighton University School of Medicine, Omaha, NE, United States
| | - Huizhan Liu
- Department of Biomedical Sciences, Creighton University School of Medicine, Omaha, NE, United States
| | - Tomoko Tateya
- Institute for Virus Research, Kyoto University, Kyoto, Japan
| | - Weiwei Guo
- Department of Otorhinolaryngology, PLA General Hospital, Beijing, China
| | - Shiming Yang
- Department of Otorhinolaryngology, PLA General Hospital, Beijing, China
| | - Kirk W Beisel
- Department of Biomedical Sciences, Creighton University School of Medicine, Omaha, NE, United States
| | - David Z Z He
- Department of Biomedical Sciences, Creighton University School of Medicine, Omaha, NE, United States
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42
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Takahashi Y, Ida H, Matsumae Y, Komaki H, Zhou Y, Kumatani A, Kanzaki M, Shiku H, Matsue T. 3D electrochemical and ion current imaging using scanning electrochemical-scanning ion conductance microscopy. Phys Chem Chem Phys 2018; 19:26728-26733. [PMID: 28951914 DOI: 10.1039/c7cp05157c] [Citation(s) in RCA: 17] [Impact Index Per Article: 2.4] [Reference Citation Analysis] [Abstract] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Indexed: 01/01/2023]
Abstract
Local cell-membrane permeability and ionic strength are important factors for maintaining the functions of cells. Here, we measured the spatial electrochemical and ion concentration profile near the sample surface with nanoscale resolution using scanning electrochemical microscopy (SECM) combined with scanning ion-conductance microscopy (SICM). The ion current feedback system is an effective way to control probe-sample distance without contact and monitor the kinetic effect of mediator regeneration and the chemical concentration profile. For demonstrating 3D electrochemical and ion concentration mapping, we evaluated the reaction rate of electrochemical mediator regeneration on an unbiased conductor and visualized inhomogeneous permeability and the ion concentration 3D profile on a single fixed adipocyte cell surface.
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Affiliation(s)
- Yasufumi Takahashi
- WPI-Advanced Institute for Materials Research, Tohoku University, 980-8577, Japan.
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43
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Bailey KA, Klymenko Y, Feist PE, Hummon AB, Stack MS, Schultz ZD. Chemical Analysis of Morphological Changes in Lysophosphatidic Acid-Treated Ovarian Cancer Cells. Sci Rep 2017; 7:15295. [PMID: 29127342 PMCID: PMC5681516 DOI: 10.1038/s41598-017-15547-7] [Citation(s) in RCA: 8] [Impact Index Per Article: 1.0] [Reference Citation Analysis] [Abstract] [MESH Headings] [Grants] [Track Full Text] [Download PDF] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Received: 07/19/2017] [Accepted: 10/30/2017] [Indexed: 12/21/2022] Open
Abstract
Ovarian cancer (OvCa) cells are reported to undergo biochemical changes at the cell surface in response to treatment with lysophosphatidic acid (LPA). Here we use scanning electron microscopy (SEM) and multiplex coherent anti-Stokes Raman scattering (CARS) imaging via supercontinuum excitation to probe morphological changes that result from LPA treatment. SEM images show distinct shedding of microvilli-like features upon treatment with LPA. Analysis of multiplex CARS images can distinguish between molecular components, such as lipids and proteins. Our results indicate that OvCa429 and SKOV3ip epithelial ovarian cancer cells undergo similar morphological and chemical responses to treatment with LPA. The microvilli-like structures on the surface of multicellular aggregates (MCAs) are removed by treatment with LPA. The CARS analysis shows a distinct decrease in protein and increase in lipid composition on the surface of LPA-treated cells. Importantly, the CARS signals from cellular sheddings from MCAs with LPA treatment are consistent with cleavage of proteins originally present. Mass spectrometry on the cellular sheddings show that a large number of proteins, both membrane and intracellular, are present. An increased number of peptides are detected for the mesenchymal cell line relative to the epithelial cell indicating a differential response to LPA treatment with cancer progression.
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Affiliation(s)
- Karen A Bailey
- Department of Chemistry and Biochemistry, University of Notre Dame, Notre Dame, IN, 46556, USA
| | - Yuliya Klymenko
- Department of Chemistry and Biochemistry, University of Notre Dame, Notre Dame, IN, 46556, USA
- Harper Cancer Research Institute, University of Notre Dame, South Bend, IN, 46617, USA
| | - Peter E Feist
- Department of Chemistry and Biochemistry, University of Notre Dame, Notre Dame, IN, 46556, USA
| | - Amanda B Hummon
- Department of Chemistry and Biochemistry, University of Notre Dame, Notre Dame, IN, 46556, USA
- Harper Cancer Research Institute, University of Notre Dame, South Bend, IN, 46617, USA
| | - M Sharon Stack
- Department of Chemistry and Biochemistry, University of Notre Dame, Notre Dame, IN, 46556, USA
- Harper Cancer Research Institute, University of Notre Dame, South Bend, IN, 46617, USA
| | - Zachary D Schultz
- Department of Chemistry and Biochemistry, University of Notre Dame, Notre Dame, IN, 46556, USA.
- Harper Cancer Research Institute, University of Notre Dame, South Bend, IN, 46617, USA.
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44
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Rheinlaender J, Schäffer TE. An Accurate Model for the Ion Current–Distance Behavior in Scanning Ion Conductance Microscopy Allows for Calibration of Pipet Tip Geometry and Tip–Sample Distance. Anal Chem 2017; 89:11875-11880. [DOI: 10.1021/acs.analchem.7b03871] [Citation(s) in RCA: 17] [Impact Index Per Article: 2.1] [Reference Citation Analysis] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Indexed: 12/16/2022]
Affiliation(s)
- Johannes Rheinlaender
- Institute of Applied Physics, University of Tübingen, Auf der Morgenstelle 10, 72076 Tübingen, Germany
| | - Tilman E. Schäffer
- Institute of Applied Physics, University of Tübingen, Auf der Morgenstelle 10, 72076 Tübingen, Germany
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45
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46
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Li D, Jacobsen MM, Rim NG, Backman D, Kaplan DL, Wong JY. Introducing biomimetic shear and ion gradients to microfluidic spinning improves silk fiber strength. Biofabrication 2017; 9:025025. [PMID: 28471354 PMCID: PMC5588659 DOI: 10.1088/1758-5090/aa711b] [Citation(s) in RCA: 13] [Impact Index Per Article: 1.6] [Reference Citation Analysis] [Abstract] [MESH Headings] [Grants] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Indexed: 11/12/2022]
Abstract
Silkworm silk is an attractive biopolymer for biomedical applications due to its high mechanical strength and biocompatibility; as a result, there is increasing interest in scalable devices to spin silk and recombinant silk so as to improve and customize their properties for diverse biomedical purposes (Vepari and Kaplan 2007 Prog. Polym. Sci. 32 ). While artificial spinning of regenerated silk fibroins adds tunability to properties such as degradation rate and surface functionalization, the resulting fibers do not yet approach the mechanical strength of native silkworm silk. These drawbacks reduce the applicability and attractiveness of artificial silk (Kinahan et al 2011 Biomacromolecules 12 ). Here, we used computational fluid dynamic simulations to incorporate shear in tandem with biomimetic ion gradients by coupling a modular novel glass microfluidic device to our previous co-axial flow device. Fibers spun with this combined apparatus demonstrated a significant increase in mechanical strength compared to fibers spun with the basic apparatus alone, with a three-fold increase in Young's modulus and extensibility and a twelve-fold increase in toughness. These results thus demonstrate the critical importance of ionic milieu and shear stress in spinning strong fibers from solubilized silk fibroin.
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Affiliation(s)
- David Li
- Department of Biomedical Engineering Boston University, 44 Cummington Mall, Boston, MA 02215, USA
| | - Matthew M. Jacobsen
- Department of Biomedical Engineering Boston University, 44 Cummington Mall, Boston, MA 02215, USA
| | - Nae Gyune Rim
- Department of Biomedical Engineering Boston University, 44 Cummington Mall, Boston, MA 02215, USA
| | - Daniel Backman
- Department of Biomedical Engineering Boston University, 44 Cummington Mall, Boston, MA 02215, USA
| | - David L. Kaplan
- Department of Biomedical Engineering, Tufts University, 4 Colby Street, Medford, MA 02155, USA
| | - Joyce Y. Wong
- Department of Biomedical Engineering Boston University, 44 Cummington Mall, Boston, MA 02215, USA
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47
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Ida H, Takahashi Y, Kumatani A, Shiku H, Matsue T. High Speed Scanning Ion Conductance Microscopy for Quantitative Analysis of Nanoscale Dynamics of Microvilli. Anal Chem 2017; 89:6015-6020. [DOI: 10.1021/acs.analchem.7b00584] [Citation(s) in RCA: 55] [Impact Index Per Article: 6.9] [Reference Citation Analysis] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Indexed: 01/02/2023]
Affiliation(s)
- Hiroki Ida
- Graduate
School of Environmental Studies, Tohoku University, Sendai, Miyagi 980-8576, Japan
| | - Yasufumi Takahashi
- Division
of Electrical Engineering and Computer Science, Kakuma-machi, Kanazawa University, Kanazawa 920-1192, Japan
- Precursory
Research for Embryonic Science and Technology (PRESTO), Japan Science and Technology Agency (JST), Saitama 332-0012, Japan
| | - Akichika Kumatani
- Graduate
School of Environmental Studies, Tohoku University, Sendai, Miyagi 980-8576, Japan
- Advanced
Institute for Material Research (AIMR), Tohoku University, Sendai, Miyagi 980-8576, Japan
| | - Hitoshi Shiku
- Department
of Applied Chemistry, Graduate School of Engineering, Tohoku University, Sendai 980-8579, Japan
| | - Tomokazu Matsue
- Graduate
School of Environmental Studies, Tohoku University, Sendai, Miyagi 980-8576, Japan
- Advanced
Institute for Material Research (AIMR), Tohoku University, Sendai, Miyagi 980-8576, Japan
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48
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Page A, Perry D, Unwin PR. Multifunctional scanning ion conductance microscopy. Proc Math Phys Eng Sci 2017; 473:20160889. [PMID: 28484332 PMCID: PMC5415692 DOI: 10.1098/rspa.2016.0889] [Citation(s) in RCA: 64] [Impact Index Per Article: 8.0] [Reference Citation Analysis] [Abstract] [Key Words] [Grants] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Received: 12/06/2016] [Accepted: 03/13/2017] [Indexed: 12/21/2022] Open
Abstract
Scanning ion conductance microscopy (SICM) is a nanopipette-based technique that has traditionally been used to image topography or to deliver species to an interface, particularly in a biological setting. This article highlights the recent blossoming of SICM into a technique with a much greater diversity of applications and capability that can be used either standalone, with advanced control (potential-time) functions, or in tandem with other methods. SICM can be used to elucidate functional information about interfaces, such as surface charge density or electrochemical activity (ion fluxes). Using a multi-barrel probe format, SICM-related techniques can be employed to deposit nanoscale three-dimensional structures and further functionality is realized when SICM is combined with scanning electrochemical microscopy (SECM), with simultaneous measurements from a single probe opening up considerable prospects for multifunctional imaging. SICM studies are greatly enhanced by finite-element method modelling for quantitative treatment of issues such as resolution, surface charge and (tip) geometry effects. SICM is particularly applicable to the study of living systems, notably single cells, although applications extend to materials characterization and to new methods of printing and nanofabrication. A more thorough understanding of the electrochemical principles and properties of SICM provides a foundation for significant applications of SICM in electrochemistry and interfacial science.
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Affiliation(s)
- Ashley Page
- Department of Chemistry, University of Warwick, Coventry CV4 7AL, UK
- MOAC Doctoral Training Centre, University of Warwick, Coventry CV4 7AL, UK
| | - David Perry
- Department of Chemistry, University of Warwick, Coventry CV4 7AL, UK
- MOAC Doctoral Training Centre, University of Warwick, Coventry CV4 7AL, UK
| | - Patrick R. Unwin
- Department of Chemistry, University of Warwick, Coventry CV4 7AL, UK
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49
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Bou G, Liu S, Sun M, Zhu J, Xue B, Guo J, Zhao Y, Qu B, Weng X, Wei Y, Lei L, Liu Z. CDX2 is essential for cell proliferation and polarity in porcine blastocysts. Development 2017; 144:1296-1306. [PMID: 28219949 DOI: 10.1242/dev.141085] [Citation(s) in RCA: 38] [Impact Index Per Article: 4.8] [Reference Citation Analysis] [Abstract] [Key Words] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Received: 06/24/2016] [Accepted: 02/03/2017] [Indexed: 01/18/2023]
Abstract
The role of CDX2 in trophectoderm (TE) cells has been extensively studied, yet the results are contradictory and species specific. Here, CDX2 expression and function were explored in early porcine embryos. Notably, siRNA-mediated gene knockdown and lentivirus-mediated TE-specific gene regulation demonstrated that CDX2 is essential for the maintenance of blastocyst integrity by regulating the BMP4-mediated blastocyst niche and classic protein kinase C (PKC)-mediated TE polarity in mammalian embryos. Mechanistically, CDX2-depleted porcine embryos stalled at the blastocyst stage and exhibited apoptosis and inactive cell proliferation, possibly resulting from BMP4 downregulation. Moreover, TE cells in CDX2-depleted blastocysts displayed defective F-actin apical organization associated with downregulation of PKCα (PRKCA). Collectively, these results provide further insight into the functional diversity of CDX2 in early mammalian embryos.
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Affiliation(s)
- Gerelchimeg Bou
- College of Life Science, Northeast Agricultural University, Harbin 150030, China.,College of Animal Science, Inner Mongolia Agricultural University, Huhhot 010018, China
| | - Shichao Liu
- College of Life Science, Northeast Agricultural University, Harbin 150030, China
| | - Mingju Sun
- College of Life Science, Northeast Agricultural University, Harbin 150030, China
| | - Jiang Zhu
- College of Life Science, Northeast Agricultural University, Harbin 150030, China
| | - Binghua Xue
- College of Life Science, Northeast Agricultural University, Harbin 150030, China
| | - Jia Guo
- College of Life Science, Northeast Agricultural University, Harbin 150030, China
| | - Yueming Zhao
- College of Life Science, Northeast Agricultural University, Harbin 150030, China
| | - Bo Qu
- Life Science and Biotechnique Research Center, Northeast Agricultural University, Harbin 150030, China
| | - Xiaogang Weng
- College of Life Science, Northeast Agricultural University, Harbin 150030, China
| | - Yanchang Wei
- College of Life Science, Northeast Agricultural University, Harbin 150030, China
| | - Lei Lei
- Department of Histology and Embryology, Harbin Medical University, Harbin 150081, China
| | - Zhonghua Liu
- College of Life Science, Northeast Agricultural University, Harbin 150030, China .,Key Laboratory of Animal Genetics, Breeding and Reproduction, Education Department of Heilongjiang Province, Harbin 150030, China
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50
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Kim SO, Kim J, Okajima T, Cho NJ. Mechanical properties of paraformaldehyde-treated individual cells investigated by atomic force microscopy and scanning ion conductance microscopy. NANO CONVERGENCE 2017; 4:5. [PMID: 28386525 PMCID: PMC5359366 DOI: 10.1186/s40580-017-0099-9] [Citation(s) in RCA: 73] [Impact Index Per Article: 9.1] [Reference Citation Analysis] [Abstract] [Key Words] [Grants] [Track Full Text] [Subscribe] [Scholar Register] [Received: 02/15/2017] [Accepted: 03/13/2017] [Indexed: 05/19/2023]
Abstract
BACKGROUND Cell fixation is an essential step to preserve cell samples for a wide range of biological assays involving histochemical and cytochemical analysis. Paraformaldehyde (PFA) has been widely used as a cross-linking fixation agent. It has been empirically recognized in a gold standard protocol that the PFA concentration for cell fixation, CPFA, is 4%. However, it is still not quantitatively clear how the conventional protocol of CPFA is optimized. METHODS Here, we investigated the mechanical properties of cell fixation as a function of CPFA by using atomic force microscopy and scanning ion conductance microscopy. The goal of this study is to investigate the effect of CPFA (0-10 wt%) on the morphological and mechanical properties of live and fixed mouse fibroblast cells. RESULTS We found that both Young's modulus, E, and the fluctuation amplitude of apical cell membrane, am, were almost constant in a lower CPFA (<10-4%). Interestingly, in an intermediate CPFA between 10-1 and 4%, E dramatically increased whereas am abruptly decreased, indicating that entire cells begin to fix at CPFA = ca. 10-1%. Moreover, these quantities were unchanged in a higher CPFA (>4%), indicating that the cell fixation is stabilized at CPFA = ca. 4%, which is consistent with the empirical concentration of cell fixation optimized in biological protocols. CONCLUSIONS Taken together, these findings offer a deeper understanding of how varying PFA concentrations influence the mechanical properties of cells and suggest new avenues for establishing refined cell fixation protocols.
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Affiliation(s)
- Seong-Oh Kim
- School of Materials Science and Engineering, Nanyang Technological University, 50 Nanyang Avenue, Singapore, 639798 Singapore
| | - Joonhui Kim
- School of Materials Science and Engineering, Nanyang Technological University, 50 Nanyang Avenue, Singapore, 639798 Singapore
| | - Takaharu Okajima
- Graduate School of Information Science and Technology, Hokkaido University, Sapporo, 060-0814 Japan
| | - Nam-Joon Cho
- School of Materials Science and Engineering, Nanyang Technological University, 50 Nanyang Avenue, Singapore, 639798 Singapore
- School of Chemical and Biomedical Engineering, Nanyang Technological University, 62 Nanyang Drive, Singapore, 637459 Singapore
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