201
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In Situ Cryo-Electron Tomography: A Post-Reductionist Approach to Structural Biology. J Mol Biol 2016; 428:332-343. [DOI: 10.1016/j.jmb.2015.09.030] [Citation(s) in RCA: 128] [Impact Index Per Article: 16.0] [Reference Citation Analysis] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Received: 08/18/2015] [Revised: 09/28/2015] [Accepted: 09/30/2015] [Indexed: 11/24/2022]
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202
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Begemann I, Viplav A, Rasch C, Galic M. Stochastic Micro-Pattern for Automated Correlative Fluorescence - Scanning Electron Microscopy. Sci Rep 2015; 5:17973. [PMID: 26647824 PMCID: PMC4673610 DOI: 10.1038/srep17973] [Citation(s) in RCA: 9] [Impact Index Per Article: 1.0] [Reference Citation Analysis] [Abstract] [Track Full Text] [Download PDF] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Received: 06/16/2015] [Accepted: 11/10/2015] [Indexed: 12/01/2022] Open
Abstract
Studies of cellular surface features gain from correlative approaches, where live cell information acquired by fluorescence light microscopy is complemented by ultrastructural information from scanning electron micrographs. Current approaches to spatially align fluorescence images with scanning electron micrographs are technically challenging and often cost or time-intensive. Relying exclusively on open-source software and equipment available in a standard lab, we have developed a method for rapid, software-assisted alignment of fluorescence images with the corresponding scanning electron micrographs via a stochastic gold micro-pattern. Here, we provide detailed instructions for micro-pattern production and image processing, troubleshooting for critical intermediate steps, and examples of membrane ultra-structures aligned with the fluorescence signal of proteins enriched at such sites. Together, the presented method for correlative fluorescence – scanning electron microscopy is versatile, robust and easily integrated into existing workflows, permitting image alignment with accuracy comparable to existing approaches with negligible investment of time or capital.
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Affiliation(s)
- Isabell Begemann
- DFG Cluster of Excellence 'Cells in Motion', (EXC 1003).,Institute of Medical Physics and Biophysics, University of Münster, Germany
| | - Abhiyan Viplav
- DFG Cluster of Excellence 'Cells in Motion', (EXC 1003).,Institute of Medical Physics and Biophysics, University of Münster, Germany
| | - Christiane Rasch
- Institute of Medical Physics and Biophysics, University of Münster, Germany
| | - Milos Galic
- DFG Cluster of Excellence 'Cells in Motion', (EXC 1003).,Institute of Medical Physics and Biophysics, University of Münster, Germany
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203
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Visualization of adherent cell monolayers by cryo-electron microscopy: A snapshot of endothelial adherens junctions. J Struct Biol 2015; 192:470-477. [DOI: 10.1016/j.jsb.2015.10.009] [Citation(s) in RCA: 2] [Impact Index Per Article: 0.2] [Reference Citation Analysis] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Received: 07/23/2015] [Revised: 10/08/2015] [Accepted: 10/09/2015] [Indexed: 01/05/2023]
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204
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Abstract
The local structure and composition of the outer membrane of an animal cell are important factors in the control of many membrane processes and mechanisms. These include signaling, sorting, and exo- and endocytic processes that are occurring all the time in a living cell. Paradoxically, not only are the local structure and composition of the membrane matters of much debate and discussion, the mechanisms that govern its genesis remain highly controversial. Here, we discuss a swathe of new technological advances that may be applied to understand the local structure and composition of the membrane of a living cell from the molecular scale to the scale of the whole membrane.
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Affiliation(s)
- Thomas S van Zanten
- National Centre for Biological Sciences (TIFR), Bellary Road, Bangalore, 560065, India
| | - Satyajit Mayor
- National Centre for Biological Sciences (TIFR), Bellary Road, Bangalore, 560065, India
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205
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Frankl A, Mari M, Reggiori F. Electron microscopy for ultrastructural analysis and protein localization in Saccharomyces cerevisiae. MICROBIAL CELL 2015; 2:412-428. [PMID: 28357267 PMCID: PMC5349205 DOI: 10.15698/mic2015.11.237] [Citation(s) in RCA: 20] [Impact Index Per Article: 2.2] [Reference Citation Analysis] [Abstract] [Key Words] [Track Full Text] [Download PDF] [Figures] [Subscribe] [Scholar Register] [Indexed: 11/13/2022]
Abstract
The yeast Saccharomyces cerevisiae is a key model system for studying of a multitude of cellular processes because of its amenability to genetics, molecular biology and biochemical procedures. Ultrastructural examinations of this organism, though, are traditionally difficult because of the presence of a thick cell wall and the high density of cytoplasmic proteins. A series of recent methodological and technical developments, however, has revived interest in morphological analyses of yeast (e.g. 123). Here we present a review of established and new methods, from sample preparation to imaging, for the ultrastructural analysis of S. cerevisiae. We include information for the use of different fixation methods, embedding procedures, approaches for contrast enhancement, and sample visualization techniques, with references to successful examples. The goal of this review is to guide researchers that want to investigate a particular process at the ultrastructural level in yeast by aiding in the selection of the most appropriate approach to visualize a specific structure or subcellular compartment.
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Affiliation(s)
- Andri Frankl
- Department of Cell Biology, University Medical Center Groningen, University of Groningen, Groningen, The Netherlands
| | - Muriel Mari
- Department of Cell Biology, University Medical Center Groningen, University of Groningen, Groningen, The Netherlands
| | - Fulvio Reggiori
- Department of Cell Biology, University Medical Center Groningen, University of Groningen, Groningen, The Netherlands
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206
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Francis MK, Holst MR, Vidal-Quadras M, Henriksson S, Santarella-Mellwig R, Sandblad L, Lundmark R. Endocytic membrane turnover at the leading edge is driven by a transient interaction between Cdc42 and GRAF1. J Cell Sci 2015; 128:4183-95. [PMID: 26446261 PMCID: PMC4712783 DOI: 10.1242/jcs.174417] [Citation(s) in RCA: 27] [Impact Index Per Article: 3.0] [Reference Citation Analysis] [Abstract] [Key Words] [Track Full Text] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Received: 05/13/2015] [Accepted: 09/28/2015] [Indexed: 12/14/2022] Open
Abstract
Changes in cell morphology require coordination of plasma membrane turnover and cytoskeleton dynamics, processes that are regulated by Rho GTPases. Here, we describe how a direct interaction between the Rho GTPase Cdc42 and the GTPase-activating protein (GAP) GRAF1 (also known as ARHGAP26), facilitates rapid cell surface turnover at the leading edge. Both Cdc42 and GRAF1 were required for fluid-phase uptake and regulated the generation of transient GRAF1-coated endocytic carriers, which were distinct from clathrin-coated vesicles. GRAF1 was found to transiently assemble at discrete Cdc42-enriched punctae at the plasma membrane, resulting in a corresponding decrease in the microdomain association of Cdc42. However, Cdc42 captured in its active state was, through a GAP-domain-mediated interaction, localised together with GRAF1 on accumulated internal structures derived from the cell surface. Correlative fluorescence and electron tomography microscopy revealed that these structures were clusters of small membrane carriers with defective endosomal processing. We conclude that a transient interaction between Cdc42 and GRAF1 drives endocytic turnover and controls the transition essential for endosomal maturation of plasma membrane internalised by this mechanism. Summary: A transient interaction between Cdc42 and GRAF1 drives endocytic turnover at the leading edge, and controls the transition essential for endosomal maturation of plasma membrane internalised by this mechanism.
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Affiliation(s)
- Monika K Francis
- Integrative Medical Biology, Umeå University, Umeå 901 87, Sweden Medical Biochemistry and Biophysics, Umeå University, Umeå 901 87, Sweden
| | - Mikkel R Holst
- Integrative Medical Biology, Umeå University, Umeå 901 87, Sweden
| | | | - Sara Henriksson
- Medical Biochemistry and Biophysics, Umeå University, Umeå 901 87, Sweden Molecular Biology, Umeå University, Umeå 901 87, Sweden
| | | | | | - Richard Lundmark
- Integrative Medical Biology, Umeå University, Umeå 901 87, Sweden Medical Biochemistry and Biophysics, Umeå University, Umeå 901 87, Sweden
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207
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O'Driscoll J, Clare D, Saibil H. Prion aggregate structure in yeast cells is determined by the Hsp104-Hsp110 disaggregase machinery. J Cell Biol 2015; 211:145-58. [PMID: 26438827 PMCID: PMC4602031 DOI: 10.1083/jcb.201505104] [Citation(s) in RCA: 24] [Impact Index Per Article: 2.7] [Reference Citation Analysis] [Abstract] [Track Full Text] [Download PDF] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Received: 05/25/2015] [Accepted: 09/08/2015] [Indexed: 12/31/2022] Open
Abstract
3D structural analysis of a yeast [PSI+] prion model by correlative fluorescence and electron tomography reveals that prion aggregate structure depends on the levels of Hsp70 chaperones, the protein remodeling ATPase Hsp104, and the Hsp70 nucleotide exchange factor/disaggregase Sse1 (yeast Hsp110). Prions consist of misfolded proteins that have adopted an infectious amyloid conformation. In vivo, prion biogenesis is intimately associated with the protein quality control machinery. Using electron tomography, we probed the effects of the heat shock protein Hsp70 chaperone system on the structure of a model yeast [PSI+] prion in situ. Individual Hsp70 deletions shift the balance between fibril assembly and disassembly, resulting in a variable shell of nonfibrillar, but still immobile, aggregates at the surface of the [PSI+] prion deposits. Both Hsp104 (an Hsp100 disaggregase) and Sse1 (the major yeast form of Hsp110) were localized to this surface shell of [PSI+] deposits in the deletion mutants. Elevation of Hsp104 expression promoted the appearance of this novel, nonfibrillar form of the prion aggregate. Moreover, Sse1 was found to regulate prion fibril length. Our studies reveal a key role for Sse1 (Hsp110), in cooperation with Hsp104, in regulating the length and assembly state of [PSI+] prion fibrils in vivo.
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Affiliation(s)
- Jonathan O'Driscoll
- Crystallography, Department of Biological Sciences, Institute of Structural and Molecular Biology, Birkbeck College, London WC1E 7HX, UK
| | - Daniel Clare
- Crystallography, Department of Biological Sciences, Institute of Structural and Molecular Biology, Birkbeck College, London WC1E 7HX, UK
| | - Helen Saibil
- Crystallography, Department of Biological Sciences, Institute of Structural and Molecular Biology, Birkbeck College, London WC1E 7HX, UK
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208
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Beckwith MS, Beckwith KS, Sikorski P, Skogaker NT, Flo TH, Halaas Ø. Seeing a Mycobacterium-Infected Cell in Nanoscale 3D: Correlative Imaging by Light Microscopy and FIB/SEM Tomography. PLoS One 2015; 10:e0134644. [PMID: 26406896 PMCID: PMC4583302 DOI: 10.1371/journal.pone.0134644] [Citation(s) in RCA: 17] [Impact Index Per Article: 1.9] [Reference Citation Analysis] [Abstract] [MESH Headings] [Track Full Text] [Download PDF] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Received: 05/11/2015] [Accepted: 07/10/2015] [Indexed: 12/13/2022] Open
Abstract
Mycobacteria pose a threat to the world health today, with pathogenic and opportunistic bacteria causing tuberculosis and non-tuberculous disease in large parts of the population. Much is still unknown about the interplay between bacteria and host during infection and disease, and more research is needed to meet the challenge of drug resistance and inefficient vaccines. This work establishes a reliable and reproducible method for performing correlative imaging of human macrophages infected with mycobacteria at an ultra-high resolution and in 3D. Focused Ion Beam/Scanning Electron Microscopy (FIB/SEM) tomography is applied, together with confocal fluorescence microscopy for localization of appropriately infected cells. The method is based on an Aclar poly(chloro-tri-fluoro)ethylene substrate, micropatterned into an advantageous geometry by a simple thermomoulding process. The platform increases the throughput and quality of FIB/SEM tomography analyses, and was successfully applied to detail the intracellular environment of a whole mycobacterium-infected macrophage in 3D.
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Affiliation(s)
- Marianne Sandvold Beckwith
- Centre of Molecular Inflammation Research, Norwegian University of Science and Technology (NTNU), Trondheim, Norway
- Department of Cancer Research and Molecular Medicine, NTNU, Trondheim, Norway
- * E-mail:
| | | | | | - Nan Tostrup Skogaker
- Department of Laboratory Medicine, Children’s and Women’s Health, NTNU, Trondheim, Norway
| | - Trude Helen Flo
- Centre of Molecular Inflammation Research, Norwegian University of Science and Technology (NTNU), Trondheim, Norway
- Department of Cancer Research and Molecular Medicine, NTNU, Trondheim, Norway
| | - Øyvind Halaas
- Department of Cancer Research and Molecular Medicine, NTNU, Trondheim, Norway
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209
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Loussert Fonta C, Humbel BM. Correlative microscopy. Arch Biochem Biophys 2015; 581:98-110. [DOI: 10.1016/j.abb.2015.05.017] [Citation(s) in RCA: 63] [Impact Index Per Article: 7.0] [Reference Citation Analysis] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Received: 03/09/2015] [Revised: 05/26/2015] [Accepted: 05/29/2015] [Indexed: 11/15/2022]
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210
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Zhang W, Cao S, Martin JL, Mueller JD, Mansky LM. Morphology and ultrastructure of retrovirus particles. AIMS BIOPHYSICS 2015; 2:343-369. [PMID: 26448965 PMCID: PMC4593330 DOI: 10.3934/biophy.2015.3.343] [Citation(s) in RCA: 38] [Impact Index Per Article: 4.2] [Reference Citation Analysis] [Abstract] [Key Words] [Track Full Text] [Download PDF] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Indexed: 11/22/2022] Open
Abstract
Retrovirus morphogenesis entails assembly of Gag proteins and the viral genome on the host plasma membrane, acquisition of the viral membrane and envelope proteins through budding, and formation of the core through the maturation process. Although in both immature and mature retroviruses, Gag and capsid proteins are organized as paracrystalline structures, the curvatures of these protein arrays are evidently not uniform within one or among all virus particles. The heterogeneity of retroviruses poses significant challenges to studying the protein contacts within the Gag and capsid lattices. This review focuses on current understanding of the molecular organization of retroviruses derived from the sub-nanometer structures of immature virus particles, helical capsid protein assemblies and soluble envelope protein complexes. These studies provide insight into the molecular elements that maintain the stability, flexibility and infectivity of virus particles. Also reviewed are morphological studies of retrovirus budding, maturation, infection and cell-cell transmission, which inform the structural transformation of the viruses and the cells during infection and viral transmission, and lead to better understanding of the interplay between the functioning viral proteins and the host cell.
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Affiliation(s)
- Wei Zhang
- Institute for Molecular Virology, University of Minnesota, Minneapolis, MN, USA ; Department of Diagnostic and Biological Sciences, School of Dentistry, University of Minnesota, Minneapolis, MN, USA ; Characterization Facility, University of Minnesota, Minneapolis, MN, USA
| | - Sheng Cao
- Wuhan Institute of Virology, Chinese Academy of Science, Wuhan, China
| | - Jessica L Martin
- Institute for Molecular Virology, University of Minnesota, Minneapolis, MN, USA ; Pharmacology Graduate Program, University of Minnesota, Minneapolis, MN, USA
| | - Joachim D Mueller
- Institute for Molecular Virology, University of Minnesota, Minneapolis, MN, USA ; School of Physics and Astronomy, University of Minnesota, Minneapolis, MN, USA
| | - Louis M Mansky
- Institute for Molecular Virology, University of Minnesota, Minneapolis, MN, USA ; Department of Diagnostic and Biological Sciences, School of Dentistry, University of Minnesota, Minneapolis, MN, USA ; Pharmacology Graduate Program, University of Minnesota, Minneapolis, MN, USA ; Department of Microbiology, University of Minnesota, Minneapolis, MN, USA
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211
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de Boer P, Hoogenboom JP, Giepmans BNG. Correlated light and electron microscopy: ultrastructure lights up! Nat Methods 2015; 12:503-13. [PMID: 26020503 DOI: 10.1038/nmeth.3400] [Citation(s) in RCA: 303] [Impact Index Per Article: 33.7] [Reference Citation Analysis] [Abstract] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Received: 08/27/2014] [Accepted: 04/15/2015] [Indexed: 12/15/2022]
Abstract
Microscopy has gone hand in hand with the study of living systems since van Leeuwenhoek observed living microorganisms and cells in 1674 using his light microscope. A spectrum of dyes and probes now enable the localization of molecules of interest within living cells by fluorescence microscopy. With electron microscopy (EM), cellular ultrastructure has been revealed. Bridging these two modalities, correlated light microscopy and EM (CLEM) opens new avenues. Studies of protein dynamics with fluorescent proteins (FPs), which leave the investigator 'in the dark' concerning cellular context, can be followed by EM examination. Rare events can be preselected at the light microscopy level before EM analysis. Ongoing development-including of dedicated probes, integrated microscopes, large-scale and three-dimensional EM and super-resolution fluorescence microscopy-now paves the way for broad CLEM implementation in biology.
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Affiliation(s)
- Pascal de Boer
- Department of Cell Biology, University Medical Center Groningen, University of Groningen, Groningen, the Netherlands
| | - Jacob P Hoogenboom
- Faculty of Applied Sciences, Delft University of Technology, Delft, the Netherlands
| | - Ben N G Giepmans
- Department of Cell Biology, University Medical Center Groningen, University of Groningen, Groningen, the Netherlands
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212
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Spronken MI, Short KR, Herfst S, Bestebroer TM, Vaes VP, van der Hoeven B, Koster AJ, Kremers GJ, Scott DP, Gultyaev AP, Sorell EM, de Graaf M, Bárcena M, Rimmelzwaan GF, Fouchier RA. Optimisations and Challenges Involved in the Creation of Various Bioluminescent and Fluorescent Influenza A Virus Strains for In Vitro and In Vivo Applications. PLoS One 2015; 10:e0133888. [PMID: 26241861 PMCID: PMC4524686 DOI: 10.1371/journal.pone.0133888] [Citation(s) in RCA: 23] [Impact Index Per Article: 2.6] [Reference Citation Analysis] [Abstract] [MESH Headings] [Grants] [Track Full Text] [Download PDF] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Received: 05/07/2015] [Accepted: 07/03/2015] [Indexed: 01/15/2023] Open
Abstract
Bioluminescent and fluorescent influenza A viruses offer new opportunities to study influenza virus replication, tropism and pathogenesis. To date, several influenza A reporter viruses have been described. These strategies typically focused on a single reporter gene (either bioluminescent or fluorescent) in a single virus backbone. However, whilst bioluminescence is suited to in vivo imaging, fluorescent viruses are more appropriate for microscopy. Therefore, the idea l reporter virus varies depending on the experiment in question, and it is important that any reporter virus strategy can be adapted accordingly. Herein, a strategy was developed to create five different reporter viruses in a single virus backbone. Specifically, enhanced green fluorescent protein (eGFP), far-red fluorescent protein (fRFP), near-infrared fluorescent protein (iRFP), Gaussia luciferase (gLUC) and firefly luciferase (fLUC) were inserted into the PA gene segment of A/PR/8/34 (H1N1). This study provides a comprehensive characterisation of the effects of different reporter genes on influenza virus replication and reporter activity. In vivo reporter gene expression, in lung tissues, was only detected for eGFP, fRFP and gLUC expressing viruses. In vitro, the eGFP-expressing virus displayed the best reporter stability and could be used for correlative light electron microscopy (CLEM). This strategy was then used to create eGFP-expressing viruses consisting entirely of pandemic H1N1, highly pathogenic avian influenza (HPAI) H5N1 and H7N9. The HPAI H5N1 eGFP-expressing virus infected mice and reporter gene expression was detected, in lung tissues, in vivo. Thus, this study provides new tools and insights for the creation of bioluminescent and fluorescent influenza A reporter viruses.
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Affiliation(s)
- Monique I. Spronken
- Department of Viroscience, Erasmus Medical Centre, Rotterdam, the Netherlands
| | - Kirsty R. Short
- Department of Viroscience, Erasmus Medical Centre, Rotterdam, the Netherlands
- School of Biomedical Sciences, University of Queensland, Brisbane, Australia
| | - Sander Herfst
- Department of Viroscience, Erasmus Medical Centre, Rotterdam, the Netherlands
| | - Theo M. Bestebroer
- Department of Viroscience, Erasmus Medical Centre, Rotterdam, the Netherlands
| | - Vincent P. Vaes
- Department of Viroscience, Erasmus Medical Centre, Rotterdam, the Netherlands
| | - Barbara van der Hoeven
- Department of Molecular Cell Biology, Section Electron Microscopy, Leiden University Medical Centre, Leiden, the Netherlands
| | - Abraham J. Koster
- Department of Molecular Cell Biology, Section Electron Microscopy, Leiden University Medical Centre, Leiden, the Netherlands
| | - Gert-Jan Kremers
- Erasmus Optical Imaging Centre, Department of Pathology, Erasmus University Medical Centre, Rotterdam, the Netherlands
| | - Dana P. Scott
- Rocky Mountain Veterinary Branch, Division of Intramural Research, National Institute of Allergy and Infectious Diseases, National Institutes of Health, Hamilton, MT, United States of America
| | - Alexander P. Gultyaev
- Department of Viroscience, Erasmus Medical Centre, Rotterdam, the Netherlands
- Leiden Institute of Advanced Computer Science, Leiden University, Leiden, the Netherlands
| | - Erin M. Sorell
- Department of Viroscience, Erasmus Medical Centre, Rotterdam, the Netherlands
- Milken Institute School of Public Health, Department of Health Policy and Management, George Washington University, Washington, DC, United States of America
| | - Miranda de Graaf
- Department of Viroscience, Erasmus Medical Centre, Rotterdam, the Netherlands
| | - Montserrat Bárcena
- Department of Molecular Cell Biology, Section Electron Microscopy, Leiden University Medical Centre, Leiden, the Netherlands
| | - Guus F. Rimmelzwaan
- Department of Viroscience, Erasmus Medical Centre, Rotterdam, the Netherlands
| | - Ron A. Fouchier
- Department of Viroscience, Erasmus Medical Centre, Rotterdam, the Netherlands
- * E-mail:
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213
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Höhn K, Fuchs J, Fröber A, Kirmse R, Glass B, Anders-Össwein M, Walther P, Kräusslich HG, Dietrich C. Preservation of protein fluorescence in embedded human dendritic cells for targeted 3D light and electron microscopy. J Microsc 2015; 259:121-128. [PMID: 25786567 PMCID: PMC4757415 DOI: 10.1111/jmi.12230] [Citation(s) in RCA: 14] [Impact Index Per Article: 1.6] [Reference Citation Analysis] [Abstract] [Key Words] [MESH Headings] [Track Full Text] [Download PDF] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Received: 09/22/2014] [Accepted: 01/28/2015] [Indexed: 11/28/2022]
Abstract
In this study, we present a correlative microscopy workflow to combine detailed 3D fluorescence light microscopy data with ultrastructural information gained by 3D focused ion beam assisted scanning electron microscopy. The workflow is based on an optimized high pressure freezing/freeze substitution protocol that preserves good ultrastructural detail along with retaining the fluorescence signal in the resin embedded specimens. Consequently, cellular structures of interest can readily be identified and imaged by state of the art 3D confocal fluorescence microscopy and are precisely referenced with respect to an imprinted coordinate system on the surface of the resin block. This allows precise guidance of the focused ion beam assisted scanning electron microscopy and limits the volume to be imaged to the structure of interest. This, in turn, minimizes the total acquisition time necessary to conduct the time consuming ultrastructural scanning electron microscope imaging while eliminating the risk to miss parts of the target structure. We illustrate the value of this workflow for targeting virus compartments, which are formed in HIV-pulsed mature human dendritic cells.
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Affiliation(s)
- K Höhn
- Department of Infectious Diseases, Virology, University Hospital Heidelberg, Heidelberg, Germany
| | - J Fuchs
- Carl Zeiss AG, Oberkochen, Germany
| | - A Fröber
- Carl Zeiss AG, Oberkochen, Germany
| | - R Kirmse
- Carl Zeiss Microscopy GmbH, Jena, Germany
| | - B Glass
- Department of Infectious Diseases, Virology, University Hospital Heidelberg, Heidelberg, Germany
| | - M Anders-Össwein
- Department of Infectious Diseases, Virology, University Hospital Heidelberg, Heidelberg, Germany
| | - P Walther
- Electron Microscopy Facility, Ulm University, Ulm, Germany
| | - H-G Kräusslich
- Department of Infectious Diseases, Virology, University Hospital Heidelberg, Heidelberg, Germany
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214
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Abstract
Advances in cell and developmental biology have often been closely linked to advances in our ability to visualize structure and function at many length and time scales. In this review, we discuss how new imaging technologies and new reagents have provided novel insights into the biology of cadherin-based cell-cell junctions. We focus on three developments: the application of super-resolution optical technologies to characterize the nanoscale organization of cadherins at cell-cell contacts, new approaches to interrogate the mechanical forces that act upon junctions, and advances in electron microscopy which have the potential to transform our understanding of cell-cell junctions.
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Affiliation(s)
- Alpha S Yap
- Division of Cell Biology and Molecular Medicine, Institute for Molecular Bioscience, The University of Queensland, St. Lucia, Brisbane, Queensland, 4072, Australia
| | - Magdalene Michael
- Division of Cell Biology and Molecular Medicine, Institute for Molecular Bioscience, The University of Queensland, St. Lucia, Brisbane, Queensland, 4072, Australia
| | - Robert G Parton
- Division of Cell Biology and Molecular Medicine, Institute for Molecular Bioscience, The University of Queensland, St. Lucia, Brisbane, Queensland, 4072, Australia
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215
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Standard fluorescent proteins as dual-modality probes for correlative experiments in an integrated light and electron microscope. J Chem Biol 2015. [DOI: 10.1007/s12154-015-0143-3] [Citation(s) in RCA: 14] [Impact Index Per Article: 1.6] [Reference Citation Analysis] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Indexed: 11/26/2022] Open
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216
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Avinoam O, Schorb M, Beese CJ, Briggs JAG, Kaksonen M. Endocytic sites mature by continuous bending and remodeling of the clathrin coat. Science 2015; 348:1369-72. [DOI: 10.1126/science.aaa9555] [Citation(s) in RCA: 191] [Impact Index Per Article: 21.2] [Reference Citation Analysis] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Indexed: 12/14/2022]
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217
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Abstract
Synapses of the mammalian CNS are diverse in size, structure, molecular composition, and function. Synapses in their myriad variations are fundamental to neural circuit development, homeostasis, plasticity, and memory storage. Unfortunately, quantitative analysis and mapping of the brain's heterogeneous synapse populations has been limited by the lack of adequate single-synapse measurement methods. Electron microscopy (EM) is the definitive means to recognize and measure individual synaptic contacts, but EM has only limited abilities to measure the molecular composition of synapses. This report describes conjugate array tomography (AT), a volumetric imaging method that integrates immunofluorescence and EM imaging modalities in voxel-conjugate fashion. We illustrate the use of conjugate AT to advance the proteometric measurement of EM-validated single-synapse analysis in a study of mouse cortex.
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218
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Heiligenstein X, Hurbain I, Delevoye C, Salamero J, Antony C, Raposo G. Step by step manipulation of the CryoCapsule with HPM high pressure freezers. Methods Cell Biol 2015; 124:259-74. [PMID: 25287845 DOI: 10.1016/b978-0-12-801075-4.00012-4] [Citation(s) in RCA: 2] [Impact Index Per Article: 0.2] [Reference Citation Analysis] [Abstract] [Key Words] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Indexed: 03/29/2023]
Abstract
The CryoCapsule is a tool dedicated to correlative light to electron microscopy experiments. Focused on simplifying the specimen manipulation throughout the entire workflow from live-cell imaging to freeze substitution following cryofixation by high pressure freezing, we introduce here a step by step procedure to use the CryoCapsule either with the high pressure freezing machines: HPM010 or the HPM100.
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Affiliation(s)
- Xavier Heiligenstein
- Centre de Recherche, Institut Curie, Paris, France; Structure and Membrane Compartments, CNRS UMR144, Paris, France
| | - Ilse Hurbain
- Centre de Recherche, Institut Curie, Paris, France; Structure and Membrane Compartments, CNRS UMR144, Paris, France; Cell and Tissue Imaging Facility (PICT-IBiSA), CNRS UMR144, Paris, France
| | - Cédric Delevoye
- Centre de Recherche, Institut Curie, Paris, France; Structure and Membrane Compartments, CNRS UMR144, Paris, France
| | - Jean Salamero
- Centre de Recherche, Institut Curie, Paris, France; Cell and Tissue Imaging Facility (PICT-IBiSA), CNRS UMR144, Paris, France; Spatio-Temporal Modeling Imaging and Cellular Dynamics, CNRS UMR144, Paris, France
| | - Claude Antony
- Department of Structural Biology and Genomics, Institut de Génétique et de Biologie Moléculaire et Cellulaire, INSERM, U964, CNRS UMR7104, Illkirch, France
| | - Graca Raposo
- Centre de Recherche, Institut Curie, Paris, France; Structure and Membrane Compartments, CNRS UMR144, Paris, France; Cell and Tissue Imaging Facility (PICT-IBiSA), CNRS UMR144, Paris, France
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219
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220
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Content delivery to newly forming Weibel-Palade bodies is facilitated by multiple connections with the Golgi apparatus. Blood 2015; 125:3509-16. [DOI: 10.1182/blood-2014-10-608596] [Citation(s) in RCA: 15] [Impact Index Per Article: 1.7] [Reference Citation Analysis] [Abstract] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Received: 10/25/2014] [Accepted: 02/21/2015] [Indexed: 11/20/2022] Open
Abstract
Key Points
WPBs stay connected to the Golgi apparatus until vesicle formation is completed. During biogenesis at the Golgi, WPBs increase in size through the addition of nontubular VWF.
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221
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Hellström K, Vihinen H, Kallio K, Jokitalo E, Ahola T. Correlative light and electron microscopy enables viral replication studies at the ultrastructural level. Methods 2015; 90:49-56. [PMID: 25916619 DOI: 10.1016/j.ymeth.2015.04.019] [Citation(s) in RCA: 18] [Impact Index Per Article: 2.0] [Reference Citation Analysis] [Abstract] [Key Words] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Received: 02/25/2015] [Revised: 04/15/2015] [Accepted: 04/17/2015] [Indexed: 02/06/2023] Open
Abstract
Electron microscopy (EM) is a powerful tool to study structural changes within cells caused e.g. by ectopic protein expression, gene silencing or virus infection. Correlative light and electron microscopy (CLEM) has proven to be useful in cases when it is problematic to identify a particular cell among a majority of unaffected cells at the EM level. In this technique the cells of interest are first identified by fluorescence microscopy and then further processed for EM. CLEM has become crucial when studying positive-strand RNA virus replication, as it takes place in nanoscale replication sites on specific cellular membranes. Here we have employed CLEM for Semliki Forest virus (SFV) replication studies both by transfecting viral replication components to cells or by infecting different cell types. For the transfection-based system, we developed an RNA template that can be detected in the cells even in the absence of replication and thus allows exploration of lethal mutations in viral proteins. In infected mammalian and mosquito cells, we were able to find replication-positive cells by using a fluorescently labeled viral protein even in the cases of low infection efficiency. The fluorescent region within these cells was shown to correspond to an area rich in modified membranes. These results show that CLEM is a valuable technique for studying virus replication and membrane modifications at the ultrastructural level.
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Affiliation(s)
- Kirsi Hellström
- Department of Food and Environmental Sciences, University of Helsinki, Helsinki, Finland
| | - Helena Vihinen
- Institute of Biotechnology, University of Helsinki, Helsinki, Finland
| | - Katri Kallio
- Department of Food and Environmental Sciences, University of Helsinki, Helsinki, Finland
| | - Eija Jokitalo
- Institute of Biotechnology, University of Helsinki, Helsinki, Finland
| | - Tero Ahola
- Department of Food and Environmental Sciences, University of Helsinki, Helsinki, Finland.
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222
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Quantitative analysis of cytoskeletal reorganization during epithelial tissue sealing by large-volume electron tomography. Nat Cell Biol 2015; 17:605-14. [DOI: 10.1038/ncb3159] [Citation(s) in RCA: 44] [Impact Index Per Article: 4.9] [Reference Citation Analysis] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Received: 03/12/2014] [Accepted: 03/13/2015] [Indexed: 12/26/2022]
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223
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Johnson E, Seiradake E, Jones EY, Davis I, Grünewald K, Kaufmann R. Correlative in-resin super-resolution and electron microscopy using standard fluorescent proteins. Sci Rep 2015; 5:9583. [PMID: 25823571 PMCID: PMC4379466 DOI: 10.1038/srep09583] [Citation(s) in RCA: 70] [Impact Index Per Article: 7.8] [Reference Citation Analysis] [Abstract] [MESH Headings] [Grants] [Track Full Text] [Download PDF] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Received: 12/04/2014] [Accepted: 03/05/2015] [Indexed: 11/15/2022] Open
Abstract
We introduce a method for correlative in-resin super-resolution fluorescence and electron microscopy (EM) of biological structures in mammalian culture cells. Cryo-fixed resin embedded samples offer superior structural preservation, performing in-resin super-resolution, however, remains a challenge. We identified key aspects of the sample preparation procedure of high pressure freezing, freeze substitution and resin embedding that are critical for preserving fluorescence and photo-switching of standard fluorescent proteins, such as mGFP, mVenus and mRuby2. This enabled us to combine single molecule localization microscopy with transmission electron microscopy imaging of standard fluorescent proteins in cryo-fixed resin embedded cells. We achieved a structural resolution of 40-50 nm (~17 nm average single molecule localization accuracy) in the fluorescence images without the use of chemical fixation or special fluorophores. Using this approach enabled the correlation of fluorescently labeled structures to the ultrastructure in the same cell at the nanometer level and superior structural preservation.
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Affiliation(s)
- Errin Johnson
- Sir William Dunn School of Pathology, University of Oxford, South Parks Road, Oxford, OX1 3RE, UK
| | - Elena Seiradake
- Division of Structural Biology, Wellcome Trust Centre for Human Genetics, University of Oxford, Roosevelt Drive, Oxford, OX3 7BN, UK
| | - E. Yvonne Jones
- Division of Structural Biology, Wellcome Trust Centre for Human Genetics, University of Oxford, Roosevelt Drive, Oxford, OX3 7BN, UK
| | - Ilan Davis
- Department of Biochemistry, University of Oxford, South Parks Road, Oxford, OX1 3QU, UK
| | - Kay Grünewald
- Division of Structural Biology, Wellcome Trust Centre for Human Genetics, University of Oxford, Roosevelt Drive, Oxford, OX3 7BN, UK
| | - Rainer Kaufmann
- Division of Structural Biology, Wellcome Trust Centre for Human Genetics, University of Oxford, Roosevelt Drive, Oxford, OX3 7BN, UK
- Department of Biochemistry, University of Oxford, South Parks Road, Oxford, OX1 3QU, UK
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224
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Suresh HG, da Silveira Dos Santos AX, Kukulski W, Tyedmers J, Riezman H, Bukau B, Mogk A. Prolonged starvation drives reversible sequestration of lipid biosynthetic enzymes and organelle reorganization in Saccharomyces cerevisiae. Mol Biol Cell 2015; 26:1601-15. [PMID: 25761633 PMCID: PMC4436773 DOI: 10.1091/mbc.e14-11-1559] [Citation(s) in RCA: 53] [Impact Index Per Article: 5.9] [Reference Citation Analysis] [Abstract] [Track Full Text] [Download PDF] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Received: 11/24/2014] [Accepted: 03/02/2015] [Indexed: 11/11/2022] Open
Abstract
Lipid homeostasis is modulated upon starvation at three different levels manifested in reversible 1) spatial confinement of lipid biosynthetic enzymes, 2) mitochondrial and endoplasmic reticular reorganization, and 3) loss of organelle contact sites, thus highlighting a novel mechanism regulating lipid biosynthesis by simply modulating flux through the pathway. Cells adapt to changing nutrient availability by modulating a variety of processes, including the spatial sequestration of enzymes, the physiological significance of which remains controversial. These enzyme deposits are claimed to represent aggregates of misfolded proteins, protein storage, or complexes with superior enzymatic activity. We monitored spatial distribution of lipid biosynthetic enzymes upon glucose depletion in Saccharomyces cerevisiae. Several different cytosolic-, endoplasmic reticulum–, and mitochondria-localized lipid biosynthetic enzymes sequester into distinct foci. Using the key enzyme fatty acid synthetase (FAS) as a model, we show that FAS foci represent active enzyme assemblies. Upon starvation, phospholipid synthesis remains active, although with some alterations, implying that other foci-forming lipid biosynthetic enzymes might retain activity as well. Thus sequestration may restrict enzymes' access to one another and their substrates, modulating metabolic flux. Enzyme sequestrations coincide with reversible drastic mitochondrial reorganization and concomitant loss of endoplasmic reticulum–mitochondria encounter structures and vacuole and mitochondria patch organelle contact sites that are reflected in qualitative and quantitative changes in phospholipid profiles. This highlights a novel mechanism that regulates lipid homeostasis without profoundly affecting the activity status of involved enzymes such that, upon entry into favorable growth conditions, cells can quickly alter lipid flux by relocalizing their enzymes.
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Affiliation(s)
- Harsha Garadi Suresh
- Center for Molecular Biology of the University of Heidelberg (ZMBH) and German Cancer Research Center (DKFZ), DKFZ-ZMBH Alliance, D-69120 Heidelberg, Germany
| | | | - Wanda Kukulski
- Structural and Computational Biology Unit and Cell Biology and Biophysics Unit, European Molecular Biology Laboratory, D-69117 Heidelberg, Germany Structural and Computational Biology Unit and Cell Biology and Biophysics Unit, European Molecular Biology Laboratory, D-69117 Heidelberg, Germany
| | - Jens Tyedmers
- Department of Medicine I and Clinical Chemistry, University of Heidelberg, D-69120 Heidelberg, Germany
| | - Howard Riezman
- NCCR Chemical Biology, Department of Biochemistry, University of Geneva, CH-1211 Geneva, Switzerland
| | - Bernd Bukau
- Center for Molecular Biology of the University of Heidelberg (ZMBH) and German Cancer Research Center (DKFZ), DKFZ-ZMBH Alliance, D-69120 Heidelberg, Germany
| | - Axel Mogk
- Center for Molecular Biology of the University of Heidelberg (ZMBH) and German Cancer Research Center (DKFZ), DKFZ-ZMBH Alliance, D-69120 Heidelberg, Germany
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225
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Li W, Stein SC, Gregor I, Enderlein J. Ultra-stable and versatile widefield cryo-fluorescence microscope for single-molecule localization with sub-nanometer accuracy. OPTICS EXPRESS 2015; 23:3770-83. [PMID: 25836229 DOI: 10.1364/oe.23.003770] [Citation(s) in RCA: 21] [Impact Index Per Article: 2.3] [Reference Citation Analysis] [Abstract] [Track Full Text] [Subscribe] [Scholar Register] [Indexed: 05/15/2023]
Abstract
We developed a stand-alone cryostat with optical access to the sample which can be adapted to any epi-fluorescence microscope for single-molecule fluorescence spectroscopy and imaging. The cryostat cools the sample to a cryogenic temperature of 89 K, and allows for imaging single molecules using an air objective with a numerical aperture of 0.7. An important property of this system is its excellent thermal and mechanical stability, enabling long-time observations of samples over several hours with negligible drift. Using this system, we performed photo-bleaching studies of Atto647N dye molecules, and find an improvement of the photostability of these molecules by more than two orders of magnitude. The resulting increased photon numbers of several millions allow for single-molecule localization accuracy of sub-nanometer.
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226
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Abstract
Endocytosis, the process whereby the plasma membrane invaginates to form vesicles, is essential for bringing many substances into the cell and for membrane turnover. The mechanism driving clathrin-mediated endocytosis (CME) involves > 50 different protein components assembling at a single location on the plasma membrane in a temporally ordered and hierarchal pathway. These proteins perform precisely choreographed steps that promote receptor recognition and clustering, membrane remodeling, and force-generating actin-filament assembly and turnover to drive membrane invagination and vesicle scission. Many critical aspects of the CME mechanism are conserved from yeast to mammals and were first elucidated in yeast, demonstrating that it is a powerful system for studying endocytosis. In this review, we describe our current mechanistic understanding of each step in the process of yeast CME, and the essential roles played by actin polymerization at these sites, while providing a historical perspective of how the landscape has changed since the preceding version of the YeastBook was published 17 years ago (1997). Finally, we discuss the key unresolved issues and where future studies might be headed.
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Affiliation(s)
- Bruce L Goode
- Brandeis University, Department of Biology, Rosenstiel Center, Waltham, Massachusetts 02454
| | - Julian A Eskin
- Brandeis University, Department of Biology, Rosenstiel Center, Waltham, Massachusetts 02454
| | - Beverly Wendland
- The Johns Hopkins University, Department of Biology, Baltimore, Maryland 21218
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227
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Serwas D, Dammermann A. Ultrastructural analysis of Caenorhabditis elegans cilia. Methods Cell Biol 2015; 129:341-367. [DOI: 10.1016/bs.mcb.2015.03.014] [Citation(s) in RCA: 9] [Impact Index Per Article: 1.0] [Reference Citation Analysis] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Indexed: 12/23/2022]
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228
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Dicer and Hsp104 function in a negative feedback loop to confer robustness to environmental stress. Cell Rep 2014; 10:47-61. [PMID: 25543137 DOI: 10.1016/j.celrep.2014.12.006] [Citation(s) in RCA: 11] [Impact Index Per Article: 1.1] [Reference Citation Analysis] [Abstract] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Received: 08/18/2014] [Revised: 11/06/2014] [Accepted: 12/02/2014] [Indexed: 11/22/2022] Open
Abstract
Epigenetic mechanisms can be influenced by environmental cues and thus evoke phenotypic variation. This plasticity can be advantageous for adaptation but also detrimental if not tightly controlled. Although having attracted considerable interest, it remains largely unknown if and how environmental cues such as temperature trigger epigenetic alterations. Using fission yeast, we demonstrate that environmentally induced discontinuous phenotypic variation is buffered by a negative feedback loop that involves the RNase Dicer and the protein disaggregase Hsp104. In the absence of Hsp104, Dicer accumulates in cytoplasmic inclusions and heterochromatin becomes unstable at elevated temperatures, an epigenetic state inherited for many cell divisions after the heat stress. Loss of Dicer leads to toxic aggregation of an exogenous prionogenic protein. Our results highlight the importance of feedback regulation in building epigenetic memory and uncover Hsp104 and Dicer as homeostatic controllers that buffer environmentally induced stochastic epigenetic variation and toxic aggregation of prionogenic proteins.
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229
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Crosstalk between PI(4,5)P₂and CK2 modulates actin polymerization during endocytic uptake. Dev Cell 2014; 30:746-58. [PMID: 25268174 DOI: 10.1016/j.devcel.2014.07.020] [Citation(s) in RCA: 15] [Impact Index Per Article: 1.5] [Reference Citation Analysis] [Abstract] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Received: 03/21/2014] [Revised: 06/13/2014] [Accepted: 07/28/2014] [Indexed: 01/02/2023]
Abstract
A transient burst of actin polymerization assists endocytic budding. How actin polymerization is controlled in this context is not understood. Here, we show that crosstalk between PI(4,5)P₂and the CK2 catalytic subunit Cka2 controls actin polymerization at endocytic sites. We find that phosphorylation of the myosin-I Myo5 by Cka2 downregulates Myo5-induced Arp2/3-dependent actin polymerization, whereas PI(4,5)P₂cooperatively relieves Myo5 autoinhibition and inhibits the catalytic activity of Cka2. Cka2 and the PI(4,5)P₂-5-phosphatases Sjl1 and Sjl2, the yeast synaptojanins, exhibit genetic interactions indicating functional redundancy. The ultrastructural analysis of plasma membrane invaginations in CK2 and synaptojanin mutants demonstrates that both cooperate to initiate constriction of the invagination neck, a process coupled to the remodeling of the endocytic actin network. Our data demonstrate a holoenzyme-independent function of CK2 in endocytic budding and establish a robust genetic, functional, and molecular link between PI(4,5)P₂and CK2, two masters of intracellular signaling.
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230
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Karreman MA, Mercier L, Schieber NL, Shibue T, Schwab Y, Goetz JG. Correlating intravital multi-photon microscopy to 3D electron microscopy of invading tumor cells using anatomical reference points. PLoS One 2014; 9:e114448. [PMID: 25479106 PMCID: PMC4257674 DOI: 10.1371/journal.pone.0114448] [Citation(s) in RCA: 45] [Impact Index Per Article: 4.5] [Reference Citation Analysis] [Abstract] [MESH Headings] [Track Full Text] [Download PDF] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Received: 08/27/2014] [Accepted: 11/06/2014] [Indexed: 01/24/2023] Open
Abstract
Correlative microscopy combines the advantages of both light and electron microscopy to enable imaging of rare and transient events at high resolution. Performing correlative microscopy in complex and bulky samples such as an entire living organism is a time-consuming and error-prone task. Here, we investigate correlative methods that rely on the use of artificial and endogenous structural features of the sample as reference points for correlating intravital fluorescence microscopy and electron microscopy. To investigate tumor cell behavior in vivo with ultrastructural accuracy, a reliable approach is needed to retrieve single tumor cells imaged deep within the tissue. For this purpose, fluorescently labeled tumor cells were subcutaneously injected into a mouse ear and imaged using two-photon-excitation microscopy. Using near-infrared branding, the position of the imaged area within the sample was labeled at the skin level, allowing for its precise recollection. Following sample preparation for electron microscopy, concerted usage of the artificial branding and anatomical landmarks enables targeting and approaching the cells of interest while serial sectioning through the specimen. We describe here three procedures showing how three-dimensional (3D) mapping of structural features in the tissue can be exploited to accurately correlate between the two imaging modalities, without having to rely on the use of artificially introduced markers of the region of interest. The methods employed here facilitate the link between intravital and nanoscale imaging of invasive tumor cells, enabling correlating function to structure in the study of tumor invasion and metastasis.
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Affiliation(s)
- Matthia A. Karreman
- European Molecular Biology Laboratory Heidelberg, Heidelberg, 69117, Germany
| | - Luc Mercier
- Inserm U1109, MN3T, Strasbourg, F-67200, France
- Université de Strasbourg, Strasbourg, F-67000, France
- LabEx Medalis, Université de Strasbourg, Strasbourg, F-67000, France
- Fédération de Médecine Translationnelle de Strasbourg (FMTS), Strasbourg, F-67000, France
| | - Nicole L. Schieber
- European Molecular Biology Laboratory Heidelberg, Heidelberg, 69117, Germany
| | - Tsukasa Shibue
- Whitehead Institute for Biomedical Research, Massachusetts Institute of Technology, Cambridge, Massachusetts, United States of America
| | - Yannick Schwab
- European Molecular Biology Laboratory Heidelberg, Heidelberg, 69117, Germany
- * E-mail: (YS); (JGG)
| | - Jacky G. Goetz
- Inserm U1109, MN3T, Strasbourg, F-67200, France
- Université de Strasbourg, Strasbourg, F-67000, France
- LabEx Medalis, Université de Strasbourg, Strasbourg, F-67000, France
- Fédération de Médecine Translationnelle de Strasbourg (FMTS), Strasbourg, F-67000, France
- * E-mail: (YS); (JGG)
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231
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Loussert Fonta C, Leis A, Mathisen C, Bouvier DS, Blanchard W, Volterra A, Lich B, Humbel BM. Analysis of acute brain slices by electron microscopy: a correlative light-electron microscopy workflow based on Tokuyasu cryo-sectioning. J Struct Biol 2014; 189:53-61. [PMID: 25448886 DOI: 10.1016/j.jsb.2014.10.011] [Citation(s) in RCA: 9] [Impact Index Per Article: 0.9] [Reference Citation Analysis] [Abstract] [Key Words] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Received: 07/18/2014] [Revised: 10/16/2014] [Accepted: 10/20/2014] [Indexed: 10/24/2022]
Abstract
Acute brain slices are slices of brain tissue that are kept vital in vitro for further recordings and analyses. This tool is of major importance in neurobiology and allows the study of brain cells such as microglia, astrocytes, neurons and their inter/intracellular communications via ion channels or transporters. In combination with light/fluorescence microscopies, acute brain slices enable the ex vivo analysis of specific cells or groups of cells inside the slice, e.g. astrocytes. To bridge ex vivo knowledge of a cell with its ultrastructure, we developed a correlative microscopy approach for acute brain slices. The workflow begins with sampling of the tissue and precise trimming of a region of interest, which contains GFP-tagged astrocytes that can be visualised by fluorescence microscopy of ultrathin sections. The astrocytes and their surroundings are then analysed by high resolution scanning transmission electron microscopy (STEM). An important aspect of this workflow is the modification of a commercial cryo-ultramicrotome to observe the fluorescent GFP signal during the trimming process. It ensured that sections contained at least one GFP astrocyte. After cryo-sectioning, a map of the GFP-expressing astrocytes is established and transferred to correlation software installed on a focused ion beam scanning electron microscope equipped with a STEM detector. Next, the areas displaying fluorescence are selected for high resolution STEM imaging. An overview area (e.g. a whole mesh of the grid) is imaged with an automated tiling and stitching process. In the final stitched image, the local organisation of the brain tissue can be surveyed or areas of interest can be magnified to observe fine details, e.g. vesicles or gold labels on specific proteins. The robustness of this workflow is contingent on the quality of sample preparation, based on Tokuyasu's protocol. This method results in a reasonable compromise between preservation of morphology and maintenance of antigenicity. Finally, an important feature of this approach is that the fluorescence of the GFP signal is preserved throughout the entire preparation process until the last step before electron microscopy.
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Affiliation(s)
- Celine Loussert Fonta
- Electron Microscopy Facility, University of Lausanne, Biophore, 1015 Lausanne, Switzerland.
| | - Andrew Leis
- CSIRO, Australian Animal Health Laboratory, Private Bag 24, Geelong 3220, Australia
| | - Cliff Mathisen
- FEI Company, Achtseweg Noord 5, 5651 GG Eindhoven, The Netherlands
| | - David S Bouvier
- Department of Fundamental Neurosciences, University of Lausanne, Rue du Bugnon 9, 1005 Lausanne, Switzerland
| | - Willy Blanchard
- Electron Microscopy Facility, University of Lausanne, Biophore, 1015 Lausanne, Switzerland
| | - Andrea Volterra
- Department of Fundamental Neurosciences, University of Lausanne, Rue du Bugnon 9, 1005 Lausanne, Switzerland
| | - Ben Lich
- FEI Company, Achtseweg Noord 5, 5651 GG Eindhoven, The Netherlands
| | - Bruno M Humbel
- Electron Microscopy Facility, University of Lausanne, Biophore, 1015 Lausanne, Switzerland
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232
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Grecchi S, Malatesta M. Visualizing endocytotic pathways at transmission electron microscopy via diaminobenzidine photo-oxidation by a fluorescent cell-membrane dye. Eur J Histochem 2014; 58:2449. [PMID: 25578976 PMCID: PMC4289848 DOI: 10.4081/ejh.2014.2449] [Citation(s) in RCA: 11] [Impact Index Per Article: 1.1] [Reference Citation Analysis] [Abstract] [Track Full Text] [Download PDF] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Received: 09/02/2014] [Revised: 09/24/2014] [Accepted: 09/25/2014] [Indexed: 12/14/2022] Open
Abstract
The endocytotic pathway involves a complex, dynamic and interacting system of intracellular compartments. PKH26 is a fluorescent dye specific for long-lasting cell membrane labelling which has been successfully used for investigating cell internalization processes, at either flow cytometry or fluorescence microscopy. In the present work, diaminobenzidine photo-oxidation was tested as a procedure to detect PKH26 dye at transmission electron microscopy. Our results demonstrated that DAB-photo-oxidation is a suitable technique to specifically visualise this fluorescent dye at the ultrastructural level: the distribution of the granular dark reaction product perfectly matches the pattern of the fluorescence staining, and the electron density of the fine precipitates makes the signal evident and precisely detectable on the different subcellular compartments involved in the plasma membrane internalization routes.
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233
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Abstract
Researchers have used transmission electron microscopy (TEM) to make contributions to cell biology for well over 50 years, and TEM continues to be an important technology in our field. We briefly present for the neophyte the components of a TEM-based study, beginning with sample preparation through imaging of the samples. We point out the limitations of TEM and issues to be considered during experimental design. Advanced electron microscopy techniques are listed as well. Finally, we point potential new users of TEM to resources to help launch their project.
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Affiliation(s)
- Mark Winey
- Molecular, Cellular, and Developmental Biology, University of Colorado at Boulder, Boulder, CO 80309 Boulder Laboratory for 3D Electron Microscopy of Cells, University of Colorado at Boulder, Boulder, CO 80309
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234
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Löschberger A, Franke C, Krohne G, van de Linde S, Sauer M. Correlative super-resolution fluorescence and electron microscopy of the nuclear pore complex with molecular resolution. J Cell Sci 2014; 127:4351-5. [PMID: 25146397 DOI: 10.1242/jcs.156620] [Citation(s) in RCA: 94] [Impact Index Per Article: 9.4] [Reference Citation Analysis] [Abstract] [Key Words] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Indexed: 01/17/2023] Open
Abstract
Here, we combine super-resolution fluorescence localization microscopy with scanning electron microscopy to map the position of proteins of nuclear pore complexes in isolated Xenopus laevis oocyte nuclear envelopes with molecular resolution in both imaging modes. We use the periodic molecular structure of the nuclear pore complex to superimpose direct stochastic optical reconstruction microscopy images with a precision of <20 nm on electron micrographs. The correlative images demonstrate quantitative molecular labeling and localization of nuclear pore complex proteins by standard immunocytochemistry with primary and secondary antibodies and reveal that the nuclear pore complex is composed of eight gp210 (also known as NUP210) protein homodimers. In addition, we find subpopulations of nuclear pore complexes with ninefold symmetry, which are found occasionally among the more typical eightfold symmetrical structures.
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Affiliation(s)
- Anna Löschberger
- Department of Biotechnology and Biophysics, Biozentrum, Julius Maximilian University Würzburg, Am Hubland, 97074 Würzburg, Germany
| | - Christian Franke
- Department of Biotechnology and Biophysics, Biozentrum, Julius Maximilian University Würzburg, Am Hubland, 97074 Würzburg, Germany
| | - Georg Krohne
- Department of Electron Microscopy, Biozentrum, Julius Maximilian University Würzburg, Am Hubland, 97074 Würzburg, Germany
| | - Sebastian van de Linde
- Department of Biotechnology and Biophysics, Biozentrum, Julius Maximilian University Würzburg, Am Hubland, 97074 Würzburg, Germany
| | - Markus Sauer
- Department of Biotechnology and Biophysics, Biozentrum, Julius Maximilian University Würzburg, Am Hubland, 97074 Würzburg, Germany
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235
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Mari M, Geerts WJ, Reggiori F. Immuno- and Correlative Light Microscopy-Electron Tomography Methods for 3D Protein Localization in Yeast. Traffic 2014; 15:1164-78. [DOI: 10.1111/tra.12192] [Citation(s) in RCA: 17] [Impact Index Per Article: 1.7] [Reference Citation Analysis] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Received: 04/30/2014] [Revised: 06/16/2014] [Accepted: 07/01/2014] [Indexed: 01/03/2023]
Affiliation(s)
- Muriel Mari
- Department of Cell Biology, Institute for Molecular Medicine; University Medical Centre Utrecht; Heidelberglaan 100 3584 CX Utrecht The Netherlands
| | - Willie J.C. Geerts
- Bijvoet Center, Faculty of Science; Utrecht University; Padualaan 8 3584 CH Utrecht The Netherlands
| | - Fulvio Reggiori
- Department of Cell Biology, Institute for Molecular Medicine; University Medical Centre Utrecht; Heidelberglaan 100 3584 CX Utrecht The Netherlands
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236
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Fukuda Y, Schrod N, Schaffer M, Feng LR, Baumeister W, Lucic V. Coordinate transformation based cryo-correlative methods for electron tomography and focused ion beam milling. Ultramicroscopy 2014; 143:15-23. [DOI: 10.1016/j.ultramic.2013.11.008] [Citation(s) in RCA: 13] [Impact Index Per Article: 1.3] [Reference Citation Analysis] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Received: 08/02/2013] [Revised: 11/18/2013] [Accepted: 11/19/2013] [Indexed: 10/25/2022]
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237
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Peddie CJ, Blight K, Wilson E, Melia C, Marrison J, Carzaniga R, Domart MC, O'Toole P, Larijani B, Collinson LM. Correlative and integrated light and electron microscopy of in-resin GFP fluorescence, used to localise diacylglycerol in mammalian cells. Ultramicroscopy 2014; 143:3-14. [PMID: 24637200 PMCID: PMC4045205 DOI: 10.1016/j.ultramic.2014.02.001] [Citation(s) in RCA: 78] [Impact Index Per Article: 7.8] [Reference Citation Analysis] [Abstract] [Key Words] [MESH Headings] [Grants] [Track Full Text] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Received: 11/19/2013] [Revised: 02/10/2014] [Accepted: 02/12/2014] [Indexed: 12/11/2022]
Abstract
Fluorescence microscopy of GFP-tagged proteins is a fundamental tool in cell biology, but without seeing the structure of the surrounding cellular space, functional information can be lost. Here we present a protocol that preserves GFP and mCherry fluorescence in mammalian cells embedded in resin with electron contrast to reveal cellular ultrastructure. Ultrathin in-resin fluorescence (IRF) sections were imaged simultaneously for fluorescence and electron signals in an integrated light and scanning electron microscope. We show, for the first time, that GFP is stable and active in resin sections in vacuo. We applied our protocol to study the subcellular localisation of diacylglycerol (DAG), a modulator of membrane morphology and membrane dynamics in nuclear envelope assembly. We show that DAG is localised to the nuclear envelope, nucleoplasmic reticulum and curved tips of the Golgi apparatus. With these developments, we demonstrate that integrated imaging is maturing into a powerful tool for accurate molecular localisation to structure.
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Affiliation(s)
- Christopher J Peddie
- Electron Microscopy Unit, London Research Institute, Cancer Research UK, London WC2A 3LY, UK
| | - Ken Blight
- Electron Microscopy Unit, London Research Institute, Cancer Research UK, London WC2A 3LY, UK
| | - Emma Wilson
- Electron Microscopy Unit, London Research Institute, Cancer Research UK, London WC2A 3LY, UK
| | - Charlotte Melia
- Electron Microscopy Unit, London Research Institute, Cancer Research UK, London WC2A 3LY, UK; Cell Biophysics Laboratory, London Research Institute, Cancer Research UK, London WC2A 3LY, UK; Department of Molecular Cell Biology, Leiden University Medical Centre, 2300 RC Leiden, The Netherlands
| | - Jo Marrison
- Department of Biology, The University of York, Heslington, York, UK
| | - Raffaella Carzaniga
- Electron Microscopy Unit, London Research Institute, Cancer Research UK, London WC2A 3LY, UK
| | - Marie-Charlotte Domart
- Electron Microscopy Unit, London Research Institute, Cancer Research UK, London WC2A 3LY, UK; Cell Biophysics Laboratory, London Research Institute, Cancer Research UK, London WC2A 3LY, UK
| | - Peter O'Toole
- Department of Biology, The University of York, Heslington, York, UK
| | - Banafshe Larijani
- Cell Biophysics Laboratory, London Research Institute, Cancer Research UK, London WC2A 3LY, UK; Cell Biophysics Laboratory, Unidad de Biofísica (CSIC-UPV/EHU),Sarriena s/n, 48940 Leioa, Spain; IKERBASQUE, Basque Foundation for Science, Bilbao, Spain
| | - Lucy M Collinson
- Electron Microscopy Unit, London Research Institute, Cancer Research UK, London WC2A 3LY, UK
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238
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Cinquin BP, Do M, McDermott G, Walters AD, Myllys M, Smith EA, Cohen-Fix O, Le Gros MA, Larabell CA. Putting molecules in their place. J Cell Biochem 2014; 115:209-16. [PMID: 23966233 DOI: 10.1002/jcb.24658] [Citation(s) in RCA: 32] [Impact Index Per Article: 3.2] [Reference Citation Analysis] [Abstract] [Key Words] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Received: 08/10/2013] [Accepted: 08/14/2013] [Indexed: 12/18/2022]
Abstract
Each class of microscope is limited to imaging specific aspects of cell structure and/or molecular organization. However, imaging the specimen by complementary microscopes and correlating the data can overcome this limitation. Whilst not a new approach, the field of correlative imaging is currently benefitting from the emergence of new microscope techniques. Here we describe the correlation of cryogenic fluorescence tomography (CFT) with soft X-ray tomography (SXT). This amalgamation of techniques integrates 3D molecular localization data (CFT) with a high-resolution, 3D cell reconstruction of the cell (SXT). Cells are imaged in both modalities in a near-native, cryopreserved state. Here we describe the current state of the art in correlative CFT-SXT, and discuss the future outlook for this method.
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Affiliation(s)
- Bertrand P Cinquin
- Department of Anatomy, University of California San Francisco, San Francisco, California
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239
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Sikirzhytski V, Magidson V, Steinman JB, He J, Le Berre M, Tikhonenko I, Ault JG, McEwen BF, Chen JK, Sui H, Piel M, Kapoor TM, Khodjakov A. Direct kinetochore-spindle pole connections are not required for chromosome segregation. ACTA ACUST UNITED AC 2014; 206:231-43. [PMID: 25023516 PMCID: PMC4107786 DOI: 10.1083/jcb.201401090] [Citation(s) in RCA: 99] [Impact Index Per Article: 9.9] [Reference Citation Analysis] [Abstract] [Track Full Text] [Download PDF] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Indexed: 12/29/2022]
Abstract
In the absence of continuous K-fiber attachment between each kinetochore and the spindle pole, one or more additional mechanisms dependent on dynein-mediated kinetochore transport exist to ensure proper chromosome segregation during mitosis. Segregation of genetic material occurs when chromosomes move to opposite spindle poles during mitosis. This movement depends on K-fibers, specialized microtubule (MT) bundles attached to the chromosomes′ kinetochores. A long-standing assumption is that continuous K-fibers connect every kinetochore to a spindle pole and the force for chromosome movement is produced at the kinetochore and coupled with MT depolymerization. However, we found that chromosomes still maintained their position at the spindle equator during metaphase and segregated properly during anaphase when one of their K-fibers was severed near the kinetochore with a laser microbeam. We also found that, in normal fully assembled spindles, K-fibers of some chromosomes did not extend to the spindle pole. These K-fibers connected to adjacent K-fibers and/or nonkinetochore MTs. Poleward movement of chromosomes with short K-fibers was uncoupled from MT depolymerization at the kinetochore. Instead, these chromosomes moved by dynein-mediated transport of the entire K-fiber/kinetochore assembly. Thus, at least two distinct parallel mechanisms drive chromosome segregation in mammalian cells.
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Affiliation(s)
| | - Valentin Magidson
- Wadsworth Center, New York State Department of Health, Albany, NY 12201
| | | | - Jie He
- Wadsworth Center, New York State Department of Health, Albany, NY 12201
| | | | - Irina Tikhonenko
- Wadsworth Center, New York State Department of Health, Albany, NY 12201
| | - Jeffrey G Ault
- Wadsworth Center, New York State Department of Health, Albany, NY 12201
| | - Bruce F McEwen
- Wadsworth Center, New York State Department of Health, Albany, NY 12201
| | | | - Haixin Sui
- Wadsworth Center, New York State Department of Health, Albany, NY 12201
| | | | | | - Alexey Khodjakov
- Wadsworth Center, New York State Department of Health, Albany, NY 12201 Rensselaer Polytechnic Institute, Troy, NY 12180
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240
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Risco C, de Castro IF, Sanz-Sánchez L, Narayan K, Grandinetti G, Subramaniam S. Three-Dimensional Imaging of Viral Infections. Annu Rev Virol 2014; 1:453-73. [PMID: 26958730 DOI: 10.1146/annurev-virology-031413-085351] [Citation(s) in RCA: 44] [Impact Index Per Article: 4.4] [Reference Citation Analysis] [Abstract] [Key Words] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Indexed: 11/09/2022]
Abstract
Three-dimensional (3D) imaging technologies are beginning to have significant impact in the field of virology, as they are helping us understand how viruses take control of cells. In this article we review several methodologies for 3D imaging of cells and show how these technologies are contributing to the study of viral infections and the characterization of specialized structures formed in virus-infected cells. We include 3D reconstruction by transmission electron microscopy (TEM) using serial sections, electron tomography, and focused ion beam scanning electron microscopy (FIB-SEM). We summarize from these methods selected contributions to our understanding of viral entry, replication, morphogenesis, egress and propagation, and changes in the spatial architecture of virus-infected cells. In combination with live-cell imaging, correlative microscopy, and new techniques for molecular mapping in situ, the availability of these methods for 3D imaging is expected to provide deeper insights into understanding the structural and dynamic aspects of viral infection.
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Affiliation(s)
- Cristina Risco
- Cell Structure Laboratory, National Center for Biotechnology (CNB-CSIC), Madrid 28049, Spain;
| | | | - Laura Sanz-Sánchez
- Cell Structure Laboratory, National Center for Biotechnology (CNB-CSIC), Madrid 28049, Spain;
| | - Kedar Narayan
- Laboratory of Cell Biology, National Cancer Institute, Bethesda, Maryland 20892;
| | - Giovanna Grandinetti
- Laboratory of Cell Biology, National Cancer Institute, Bethesda, Maryland 20892;
| | - Sriram Subramaniam
- Laboratory of Cell Biology, National Cancer Institute, Bethesda, Maryland 20892;
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241
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Xiong H, Zhou Z, Zhu M, Lv X, Li A, Li S, Li L, Yang T, Wang S, Yang Z, Xu T, Luo Q, Gong H, Zeng S. Chemical reactivation of quenched fluorescent protein molecules enables resin-embedded fluorescence microimaging. Nat Commun 2014; 5:3992. [PMID: 24886825 PMCID: PMC4059927 DOI: 10.1038/ncomms4992] [Citation(s) in RCA: 77] [Impact Index Per Article: 7.7] [Reference Citation Analysis] [Abstract] [Track Full Text] [Download PDF] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Received: 08/21/2013] [Accepted: 04/29/2014] [Indexed: 11/09/2022] Open
Abstract
Resin embedding is a well-established technique to prepare biological specimens for microscopic imaging. However, it is not compatible with modern green-fluorescent protein (GFP) fluorescent-labelling technique because it significantly quenches the fluorescence of GFP and its variants. Previous empirical optimization efforts are good for thin tissue but not successful on macroscopic tissue blocks as the quenching mechanism remains uncertain. Here we show most of the quenched GFP molecules are structurally preserved and not denatured after routine embedding in resin, and can be chemically reactivated to a fluorescent state by alkaline buffer during imaging. We observe up to 98% preservation in yellow-fluorescent protein case, and improve the fluorescence intensity 11.8-fold compared with unprocessed samples. We demonstrate fluorescence microimaging of resin-embedded EGFP/EYFP-labelled tissue block without noticeable loss of labelled structures. This work provides a turning point for the imaging of fluorescent protein-labelled specimens after resin embedding. Resin embedding of specimens is widely used for microscopy but can cause the loss of fluorescence from green-fluorescent protein. Here, the authors show that these proteins can be reactivated in resin-embedded samples through the use of alkaline buffer.
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Affiliation(s)
- Hanqing Xiong
- 1] Britton Chance Center for Biomedical Photonics, Wuhan National Laboratory for Optoelectronics-Huazhong University of Science and Technology, Wuhan 430074, China [2] Department of Biomedical Engineering, Key Laboratory of Biomedical Photonics of Ministry of Education, Huazhong University of Science and Technology, Wuhan 430074, China
| | - Zhenqiao Zhou
- 1] Britton Chance Center for Biomedical Photonics, Wuhan National Laboratory for Optoelectronics-Huazhong University of Science and Technology, Wuhan 430074, China [2] Department of Biomedical Engineering, Key Laboratory of Biomedical Photonics of Ministry of Education, Huazhong University of Science and Technology, Wuhan 430074, China
| | - Mingqiang Zhu
- Britton Chance Center for Biomedical Photonics, Wuhan National Laboratory for Optoelectronics-Huazhong University of Science and Technology, Wuhan 430074, China
| | - Xiaohua Lv
- 1] Britton Chance Center for Biomedical Photonics, Wuhan National Laboratory for Optoelectronics-Huazhong University of Science and Technology, Wuhan 430074, China [2] Department of Biomedical Engineering, Key Laboratory of Biomedical Photonics of Ministry of Education, Huazhong University of Science and Technology, Wuhan 430074, China
| | - Anan Li
- 1] Britton Chance Center for Biomedical Photonics, Wuhan National Laboratory for Optoelectronics-Huazhong University of Science and Technology, Wuhan 430074, China [2] Department of Biomedical Engineering, Key Laboratory of Biomedical Photonics of Ministry of Education, Huazhong University of Science and Technology, Wuhan 430074, China
| | - Shiwei Li
- 1] Britton Chance Center for Biomedical Photonics, Wuhan National Laboratory for Optoelectronics-Huazhong University of Science and Technology, Wuhan 430074, China [2] Department of Biomedical Engineering, Key Laboratory of Biomedical Photonics of Ministry of Education, Huazhong University of Science and Technology, Wuhan 430074, China
| | - Longhui Li
- 1] Britton Chance Center for Biomedical Photonics, Wuhan National Laboratory for Optoelectronics-Huazhong University of Science and Technology, Wuhan 430074, China [2] Department of Biomedical Engineering, Key Laboratory of Biomedical Photonics of Ministry of Education, Huazhong University of Science and Technology, Wuhan 430074, China
| | - Tao Yang
- 1] Britton Chance Center for Biomedical Photonics, Wuhan National Laboratory for Optoelectronics-Huazhong University of Science and Technology, Wuhan 430074, China [2] Department of Biomedical Engineering, Key Laboratory of Biomedical Photonics of Ministry of Education, Huazhong University of Science and Technology, Wuhan 430074, China
| | - Siming Wang
- 1] Britton Chance Center for Biomedical Photonics, Wuhan National Laboratory for Optoelectronics-Huazhong University of Science and Technology, Wuhan 430074, China [2] Department of Biomedical Engineering, Key Laboratory of Biomedical Photonics of Ministry of Education, Huazhong University of Science and Technology, Wuhan 430074, China
| | - Zhongqin Yang
- 1] Britton Chance Center for Biomedical Photonics, Wuhan National Laboratory for Optoelectronics-Huazhong University of Science and Technology, Wuhan 430074, China [2] Department of Biomedical Engineering, Key Laboratory of Biomedical Photonics of Ministry of Education, Huazhong University of Science and Technology, Wuhan 430074, China
| | - Tonghui Xu
- 1] Britton Chance Center for Biomedical Photonics, Wuhan National Laboratory for Optoelectronics-Huazhong University of Science and Technology, Wuhan 430074, China [2] Department of Biomedical Engineering, Key Laboratory of Biomedical Photonics of Ministry of Education, Huazhong University of Science and Technology, Wuhan 430074, China
| | - Qingming Luo
- 1] Britton Chance Center for Biomedical Photonics, Wuhan National Laboratory for Optoelectronics-Huazhong University of Science and Technology, Wuhan 430074, China [2] Department of Biomedical Engineering, Key Laboratory of Biomedical Photonics of Ministry of Education, Huazhong University of Science and Technology, Wuhan 430074, China
| | - Hui Gong
- 1] Britton Chance Center for Biomedical Photonics, Wuhan National Laboratory for Optoelectronics-Huazhong University of Science and Technology, Wuhan 430074, China [2] Department of Biomedical Engineering, Key Laboratory of Biomedical Photonics of Ministry of Education, Huazhong University of Science and Technology, Wuhan 430074, China
| | - Shaoqun Zeng
- 1] Britton Chance Center for Biomedical Photonics, Wuhan National Laboratory for Optoelectronics-Huazhong University of Science and Technology, Wuhan 430074, China [2] Department of Biomedical Engineering, Key Laboratory of Biomedical Photonics of Ministry of Education, Huazhong University of Science and Technology, Wuhan 430074, China
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242
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Peddie CJ, Collinson LM. Exploring the third dimension: Volume electron microscopy comes of age. Micron 2014; 61:9-19. [DOI: 10.1016/j.micron.2014.01.009] [Citation(s) in RCA: 245] [Impact Index Per Article: 24.5] [Reference Citation Analysis] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Received: 12/17/2013] [Revised: 01/30/2014] [Accepted: 01/30/2014] [Indexed: 12/12/2022]
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243
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Heiligenstein X, Heiligenstein J, Delevoye C, Hurbain I, Bardin S, Paul-Gilloteaux P, Sengmanivong L, Régnier G, Salamero J, Antony C, Raposo G. The CryoCapsule: simplifying correlative light to electron microscopy. Traffic 2014; 15:700-16. [PMID: 24533564 PMCID: PMC4064126 DOI: 10.1111/tra.12164] [Citation(s) in RCA: 29] [Impact Index Per Article: 2.9] [Reference Citation Analysis] [Abstract] [Key Words] [MESH Headings] [Grants] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Received: 08/28/2013] [Revised: 02/12/2014] [Accepted: 02/17/2014] [Indexed: 11/28/2022]
Abstract
Correlating complementary multiple scale images of the same object is a straightforward means to decipher biological processes. Light microscopy and electron microscopy are the most commonly used imaging techniques, yet despite their complementarity, the experimental procedures available to correlate them are technically complex. We designed and manufactured a new device adapted to many biological specimens, the CryoCapsule, that simplifies the multiple sample preparation steps, which at present separate live cell fluorescence imaging from contextual high-resolution electron microscopy, thus opening new strategies for full correlative light to electron microscopy. We tested the biological application of this highly optimized tool on three different specimens: the in vitro Xenopus laevis mitotic spindle, melanoma cells over-expressing YFP-langerin sequestered in organized membranous subcellular organelles and a pigmented melanocytic cell in which the endosomal system was labeled with internalized fluorescent transferrin.
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Affiliation(s)
- Xavier Heiligenstein
- Institut Curie, Centre de Recherche, Paris 75248, France
- Structure and Membrane Compartments, CNRS UMR144, Paris 75248, France
| | - Jérôme Heiligenstein
- Processes and Engineering in Mechanics and Materials, Centre National de la Recherche Scientifique (CNRS), UMR 8006, CER de Paris, Arts et Métiers ParisTech, Paris, France
- CryoCapCell, 75015 Paris, France
| | - Cédric Delevoye
- Institut Curie, Centre de Recherche, Paris 75248, France
- Structure and Membrane Compartments, CNRS UMR144, Paris 75248, France
| | - Ilse Hurbain
- Institut Curie, Centre de Recherche, Paris 75248, France
- Structure and Membrane Compartments, CNRS UMR144, Paris 75248, France
- Cell and Tissue Imaging Facility (PICT-IBiSA), CNRS UMR144, Paris 75248, France
| | - Sabine Bardin
- Institut Curie, Centre de Recherche, Paris 75248, France
- Molecular Mechanisms of Intracellular Transport, CNRS UMR144, Paris 75248, France
| | - Perrine Paul-Gilloteaux
- Institut Curie, Centre de Recherche, Paris 75248, France
- Spatio-temporal modeling Imaging and cellular dynamics, CNRS UMR144, Paris 75248, France
- Cell and Tissue Imaging Facility (PICT-IBiSA), CNRS UMR144, Paris 75248, France
| | - Lucie Sengmanivong
- Institut Curie, Centre de Recherche, Paris 75248, France
- Spatio-temporal modeling Imaging and cellular dynamics, CNRS UMR144, Paris 75248, France
- Cell and Tissue Imaging Facility (PICT-IBiSA), CNRS UMR144, Paris 75248, France
| | - Gilles Régnier
- Processes and Engineering in Mechanics and Materials, Centre National de la Recherche Scientifique (CNRS), UMR 8006, CER de Paris, Arts et Métiers ParisTech, Paris, France
| | - Jean Salamero
- Institut Curie, Centre de Recherche, Paris 75248, France
- Spatio-temporal modeling Imaging and cellular dynamics, CNRS UMR144, Paris 75248, France
- Cell and Tissue Imaging Facility (PICT-IBiSA), CNRS UMR144, Paris 75248, France
| | - Claude Antony
- Department of Structural Biology and Genomics, Institut de Génétique et de Biologie Moléculaire et Cellulaire, INSERM, U964, CNRS, UMR7104, Illkirch BP10142, France
| | - Graca Raposo
- Institut Curie, Centre de Recherche, Paris 75248, France
- Structure and Membrane Compartments, CNRS UMR144, Paris 75248, France
- Cell and Tissue Imaging Facility (PICT-IBiSA), CNRS UMR144, Paris 75248, France
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244
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Giss D, Kemmerling S, Dandey V, Stahlberg H, Braun T. Exploring the Interactome: Microfluidic Isolation of Proteins and Interacting Partners for Quantitative Analysis by Electron Microscopy. Anal Chem 2014; 86:4680-7. [DOI: 10.1021/ac4027803] [Citation(s) in RCA: 10] [Impact Index Per Article: 1.0] [Reference Citation Analysis] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Indexed: 12/25/2022]
Affiliation(s)
- Dominic Giss
- Center
for Cellular Imaging
and Nano Analytics, Biozentrum, University of Basel, Basel 4056, Switzerland
| | - Simon Kemmerling
- Center
for Cellular Imaging
and Nano Analytics, Biozentrum, University of Basel, Basel 4056, Switzerland
| | - Venkata Dandey
- Center
for Cellular Imaging
and Nano Analytics, Biozentrum, University of Basel, Basel 4056, Switzerland
| | - Henning Stahlberg
- Center
for Cellular Imaging
and Nano Analytics, Biozentrum, University of Basel, Basel 4056, Switzerland
| | - Thomas Braun
- Center
for Cellular Imaging
and Nano Analytics, Biozentrum, University of Basel, Basel 4056, Switzerland
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245
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Padman BS, Bach M, Ramm G. An improved procedure for subcellular spatial alignment during live-cell CLEM. PLoS One 2014; 9:e95967. [PMID: 24755651 PMCID: PMC3995996 DOI: 10.1371/journal.pone.0095967] [Citation(s) in RCA: 14] [Impact Index Per Article: 1.4] [Reference Citation Analysis] [Abstract] [MESH Headings] [Track Full Text] [Download PDF] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Received: 01/13/2014] [Accepted: 03/31/2014] [Indexed: 11/18/2022] Open
Abstract
Live-cell correlative light and electron microscopy (CLEM) offers unique insights into the ultrastructure of dynamic cellular processes. A critical and technically challenging part of CLEM is the 3-dimensional relocation of the intracellular region of interest during sample processing. We have developed a simple CLEM procedure that uses toner particles from a laser printer as orientation marks. This facilitates easy tracking of a region of interest even by eye throughout the whole procedure. Combined with subcellular fluorescence markers for the plasma membrane and nucleus, the toner particles allow for precise subcellular spatial alignment of the optical and electron microscopy data sets. The toner-based reference grid is printed and transferred onto a polymer film using a standard office printer and laminator. We have also designed a polymer film holder that is compatible with most inverted microscopes, and have validated our strategy by following the ultrastructure of mitochondria that were selectively photo-irradiated during live-cell microscopy. In summary, our inexpensive and robust CLEM procedure simplifies optical imaging, without limiting the choice of optical microscope.
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Affiliation(s)
- Benjamin S. Padman
- Department of Biochemistry and Molecular Biology, Monash University, Clayton campus, Victoria, Australia
- Monash Micro Imaging, Monash University, Clayton campus, Victoria, Australia
| | - Markus Bach
- Department of Biochemistry and Molecular Biology, Monash University, Clayton campus, Victoria, Australia
- Monash Micro Imaging, Monash University, Clayton campus, Victoria, Australia
| | - Georg Ramm
- Department of Biochemistry and Molecular Biology, Monash University, Clayton campus, Victoria, Australia
- Monash Micro Imaging, Monash University, Clayton campus, Victoria, Australia
- * E-mail:
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246
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Perkovic M, Kunz M, Endesfelder U, Bunse S, Wigge C, Yu Z, Hodirnau VV, Scheffer MP, Seybert A, Malkusch S, Schuman EM, Heilemann M, Frangakis AS. Correlative light- and electron microscopy with chemical tags. J Struct Biol 2014; 186:205-13. [PMID: 24698954 DOI: 10.1016/j.jsb.2014.03.018] [Citation(s) in RCA: 52] [Impact Index Per Article: 5.2] [Reference Citation Analysis] [Abstract] [Key Words] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Received: 02/19/2014] [Revised: 03/20/2014] [Accepted: 03/24/2014] [Indexed: 10/25/2022]
Abstract
Correlative microscopy incorporates the specificity of fluorescent protein labeling into high-resolution electron micrographs. Several approaches exist for correlative microscopy, most of which have used the green fluorescent protein (GFP) as the label for light microscopy. Here we use chemical tagging and synthetic fluorophores instead, in order to achieve protein-specific labeling, and to perform multicolor imaging. We show that synthetic fluorophores preserve their post-embedding fluorescence in the presence of uranyl acetate. Post-embedding fluorescence is of such quality that the specimen can be prepared with identical protocols for scanning electron microscopy (SEM) and transmission electron microscopy (TEM); this is particularly valuable when singular or otherwise difficult samples are examined. We show that synthetic fluorophores give bright, well-resolved signals in super-resolution light microscopy, enabling us to superimpose light microscopic images with a precision of up to 25 nm in the x-y plane on electron micrographs. To exemplify the preservation quality of our new method we visualize the molecular arrangement of cadherins in adherens junctions of mouse epithelial cells.
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Affiliation(s)
- Mario Perkovic
- Goethe University Frankfurt, Buchmann Institute for Molecular Life Sciences and Institute for Biophysics, Max-von-Laue Str. 15, 60438 Frankfurt am Main, Germany
| | - Michael Kunz
- Goethe University Frankfurt, Buchmann Institute for Molecular Life Sciences and Institute for Biophysics, Max-von-Laue Str. 15, 60438 Frankfurt am Main, Germany
| | - Ulrike Endesfelder
- Goethe University Frankfurt, Institute for Physical and Theoretical Chemistry, Max-von-Laue Str. 13, 60438 Frankfurt am Main, Germany
| | - Stefanie Bunse
- Max-Planck-Institute for Brain Research, Max-von-Laue Str. 4, 60438 Frankfurt am Main, Germany
| | - Christoph Wigge
- Goethe University Frankfurt, Buchmann Institute for Molecular Life Sciences and Institute for Biophysics, Max-von-Laue Str. 15, 60438 Frankfurt am Main, Germany
| | - Zhou Yu
- Goethe University Frankfurt, Buchmann Institute for Molecular Life Sciences and Institute for Biophysics, Max-von-Laue Str. 15, 60438 Frankfurt am Main, Germany
| | - Victor-Valentin Hodirnau
- Goethe University Frankfurt, Buchmann Institute for Molecular Life Sciences and Institute for Biophysics, Max-von-Laue Str. 15, 60438 Frankfurt am Main, Germany
| | - Margot P Scheffer
- Goethe University Frankfurt, Buchmann Institute for Molecular Life Sciences and Institute for Biophysics, Max-von-Laue Str. 15, 60438 Frankfurt am Main, Germany
| | - Anja Seybert
- Goethe University Frankfurt, Buchmann Institute for Molecular Life Sciences and Institute for Biophysics, Max-von-Laue Str. 15, 60438 Frankfurt am Main, Germany
| | - Sebastian Malkusch
- Goethe University Frankfurt, Institute for Physical and Theoretical Chemistry, Max-von-Laue Str. 13, 60438 Frankfurt am Main, Germany
| | - Erin M Schuman
- Max-Planck-Institute for Brain Research, Max-von-Laue Str. 4, 60438 Frankfurt am Main, Germany
| | - Mike Heilemann
- Goethe University Frankfurt, Institute for Physical and Theoretical Chemistry, Max-von-Laue Str. 13, 60438 Frankfurt am Main, Germany
| | - Achilleas S Frangakis
- Goethe University Frankfurt, Buchmann Institute for Molecular Life Sciences and Institute for Biophysics, Max-von-Laue Str. 15, 60438 Frankfurt am Main, Germany.
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247
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McDonald KL. Out with the old and in with the new: rapid specimen preparation procedures for electron microscopy of sectioned biological material. PROTOPLASMA 2014; 251:429-448. [PMID: 24258967 DOI: 10.1007/s00709-013-0575-y] [Citation(s) in RCA: 55] [Impact Index Per Article: 5.5] [Reference Citation Analysis] [Abstract] [MESH Headings] [Track Full Text] [Subscribe] [Scholar Register] [Received: 10/21/2013] [Accepted: 10/22/2013] [Indexed: 06/02/2023]
Abstract
This article presents the best current practices for preparation of biological samples for examination as thin sections in an electron microscope. The historical development of fixation, dehydration, and embedding procedures for biological materials are reviewed for both conventional and low temperature methods. Conventional procedures for processing cells and tissues are usually done over days and often produce distortions, extractions, and other artifacts that are not acceptable for today's structural biology standards. High-pressure freezing and freeze substitution can minimize some of these artifacts. New methods that reduce the times for freeze substitution and resin embedding to a few hours are discussed as well as a new rapid room temperature method for preparing cells for on-section immunolabeling without the use of aldehyde fixatives.
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Affiliation(s)
- Kent L McDonald
- Electron Microscope Laboratory, University of California, 26 Giannini Hall, Berkeley, CA, 94720, USA,
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248
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Tubular endocytosis drives remodelling of the apical surface during epithelial morphogenesis in Drosophila. Nat Commun 2014; 4:2244. [PMID: 23921440 PMCID: PMC3753550 DOI: 10.1038/ncomms3244] [Citation(s) in RCA: 81] [Impact Index Per Article: 8.1] [Reference Citation Analysis] [Abstract] [Track Full Text] [Download PDF] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Received: 04/05/2013] [Accepted: 07/04/2013] [Indexed: 11/23/2022] Open
Abstract
During morphogenesis, remodelling of cell shape requires the expansion or contraction of plasma membrane domains. Here we identify a mechanism underlying the restructuring of the apical surface during epithelial morphogenesis in Drosophila. We show that the retraction of villous protrusions and subsequent apical plasma membrane flattening is an endocytosis-driven morphogenetic process. Quantitation of endogenously tagged GFP::Rab5 dynamics reveals a massive increase in apical endocytosis that correlates with changes in apical morphology. This increase is accompanied by the formation of tubular plasma membrane invaginations that serve as platforms for the de novo generation of Rab5-positive endosomes. We identify the Rab5-effector Rabankyrin-5 as a regulator of this pathway and demonstrate that blocking dynamin activity results in the complete inhibition of tubular endocytosis, in the disappearance of Rab5 endosomes, and in the inhibition of surface flattening. These data collectively demonstrate a requirement for endocytosis in morphogenetic remodelling during epithelial development. During epithelial morphogenesis in Drosophila, the villous apical cell surface is flattened. Fabrowski et al. show that this flattening depends on a dramatic increase in endocytosis associated with the formation of tubular invaginations, revealing a role for membrane trafficking in morphological remodelling.
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249
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Yuan Y, Li M, Hong N, Hong Y. Correlative light and electron microscopic analyses of mitochondrial distribution in blastomeres of early fish embryos. FASEB J 2014; 28:577-585. [DOI: 10.1096/fj.13-233635] [Citation(s) in RCA: 10] [Impact Index Per Article: 1.0] [Reference Citation Analysis] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Indexed: 08/30/2023]
Affiliation(s)
- Yongming Yuan
- Department of Biological SciencesNational University of SingaporeSingaporeSingapore
| | - Mingyou Li
- Department of Biological SciencesNational University of SingaporeSingaporeSingapore
- College of Fisheries and Life ScienceShanghai Ocean UniversityShanghaiChina
| | - Ni Hong
- Department of Biological SciencesNational University of SingaporeSingaporeSingapore
| | - Yunhan Hong
- Department of Biological SciencesNational University of SingaporeSingaporeSingapore
- College of Fisheries and Life ScienceShanghai Ocean UniversityShanghaiChina
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250
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Idrissi FZ, Geli MI. Zooming in on the molecular mechanisms of endocytic budding by time-resolved electron microscopy. Cell Mol Life Sci 2014; 71:641-57. [PMID: 24002236 PMCID: PMC11113444 DOI: 10.1007/s00018-013-1452-8] [Citation(s) in RCA: 19] [Impact Index Per Article: 1.9] [Reference Citation Analysis] [Abstract] [Key Words] [MESH Headings] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Received: 05/21/2013] [Revised: 07/17/2013] [Accepted: 08/08/2013] [Indexed: 12/31/2022]
Abstract
Endocytic budding implies the remodeling of a plasma membrane portion from a flat sheet to a closed vesicle. Clathrin- and actin-mediated endocytosis in yeast has proven a very powerful model to study this process, with more than 60 evolutionarily conserved proteins involved in fashioning primary endocytic vesicles. Major progress in the field has been made during the last decades by defining the sequential recruitment of the endocytic machinery at the cell cortex using live-cell fluorescence microscopy. Higher spatial resolution has been recently achieved by developing time-resolved electron microscopy methods, allowing for the first time the visualization of changes in the plasma membrane shape, coupled to the dynamics of the endocytic machinery. Here, we highlight these advances and review recent findings from yeast and mammals that have increased our understanding of where and how endocytic proteins may apply force to remodel the plasma membrane during different stages of the process.
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Affiliation(s)
- Fatima-Zahra Idrissi
- Department of Cell Biology, Instituto de Biología Molecular de Barcelona (CSIC), Baldiri i Reixac 15, 08028, Barcelona, Spain,
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