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Crabtree A, Neikirk K, Pinette JA, Whiteside A, Shao B, Bedenbaugh J, Vue Z, Vang L, Le H, Demirci M, Ahmad T, Owens TC, Oliver A, Zeleke F, Beasley HK, Lopez EG, Scudese E, Rodman T, Kabugi K, Koh A, Navarro S, Lam J, Kirk B, Mungai M, Sweetwyne M, Koh HJ, Zaganjor E, Damo SM, Gaddy JA, Kirabo A, Murray SA, Cooper A, Williams C, McReynolds MR, Marshall AG, Hinton A. Quantitative assessment of morphological changes in lipid droplets and lipid-mito interactions with aging in brown adipose. J Cell Physiol 2024. [PMID: 39138923 DOI: 10.1002/jcp.31340] [Citation(s) in RCA: 0] [Impact Index Per Article: 0] [Reference Citation Analysis] [Abstract] [Key Words] [Grants] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Received: 09/23/2023] [Revised: 05/26/2024] [Accepted: 06/04/2024] [Indexed: 08/15/2024]
Abstract
The physical characteristics of brown adipose tissue (BAT) are defined by the presence of multilocular lipid droplets (LDs) within the brown adipocytes and a high abundance of iron-containing mitochondria, which give it its characteristic color. Normal mitochondrial function is, in part, regulated by organelle-to-organelle contacts. For example, the contact sites that mediate mitochondria-LD interactions are thought to have various physiological roles, such as the synthesis and metabolism of lipids. Aging is associated with mitochondrial dysfunction, and previous studies show that there are changes in mitochondrial structure and the proteins that modulate organelle contact sites. However, how mitochondria-LD interactions change with aging has yet to be fully clarified. Therefore, we sought to define age-related changes in LD morphology and mitochondria-lipid interactions in BAT. We examined the three-dimensional morphology of mitochondria and LDs in young (3-month) and aged (2-year) murine BAT using serial block face-scanning electron microscopy and the Amira program for segmentation, analysis, and quantification. Our analyses showed reductions in LD volume, area, and perimeter in aged samples in comparison to young samples. Additionally, we observed changes in LD appearance and type in aged samples compared to young samples. Notably, we found differences in mitochondrial interactions with LDs, which could implicate that these contacts may be important for energetics in aging. Upon further investigation, we also found changes in mitochondrial and cristae structure for the mitochondria interacting with LDs. Overall, these data define the nature of LD morphology and organelle-organelle contacts during aging and provide insight into LD contact site changes that interconnect biogerontology with mitochondrial function, metabolism, and bioactivity in aged BAT.
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Affiliation(s)
- Amber Crabtree
- Department of Molecular Physiology and Biophysics, Vanderbilt University, Nashville, Tennessee, USA
- The Frist Center for Autism and Innovation, Vanderbilt University, Nashville, Tennessee, USA
| | - Kit Neikirk
- Department of Molecular Physiology and Biophysics, Vanderbilt University, Nashville, Tennessee, USA
| | - Julia A Pinette
- Department of Molecular Physiology and Biophysics, Vanderbilt University, Nashville, Tennessee, USA
| | - Aaron Whiteside
- Department of Molecular Physiology and Biophysics, Vanderbilt University, Nashville, Tennessee, USA
| | - Bryanna Shao
- Department of Molecular Physiology and Biophysics, Vanderbilt University, Nashville, Tennessee, USA
| | - Jessica Bedenbaugh
- Department of Molecular Physiology and Biophysics, Vanderbilt University, Nashville, Tennessee, USA
| | - Zer Vue
- Department of Molecular Physiology and Biophysics, Vanderbilt University, Nashville, Tennessee, USA
| | - Larry Vang
- Department of Molecular Physiology and Biophysics, Vanderbilt University, Nashville, Tennessee, USA
| | - Han Le
- Department of Molecular Physiology and Biophysics, Vanderbilt University, Nashville, Tennessee, USA
| | - Mert Demirci
- Department of Medicine, Division Nephrology and Hypertension, Vanderbilt University Medical Center, Nashville, Tennessee, USA
| | - Taseer Ahmad
- Department of Medicine, Division of Clinical Pharmacology, Vanderbilt University Medical Center, Nashville, Tennessee, USA
- Department of Pharmacology, College of Pharmacy, University of Sargodha, Sargodha, Punjab, Pakistan
| | - Trinity Celeste Owens
- Department of Molecular Physiology and Biophysics, Vanderbilt University, Nashville, Tennessee, USA
| | - Ashton Oliver
- Department of Molecular Physiology and Biophysics, Vanderbilt University, Nashville, Tennessee, USA
| | - Faben Zeleke
- Department of Molecular Physiology and Biophysics, Vanderbilt University, Nashville, Tennessee, USA
| | - Heather K Beasley
- Department of Molecular Physiology and Biophysics, Vanderbilt University, Nashville, Tennessee, USA
| | - Edgar Garza Lopez
- Department of Internal Medicine, University of Iowa, Iowa City, Iowa, USA
| | - Estevão Scudese
- Department of Molecular Physiology and Biophysics, Vanderbilt University, Nashville, Tennessee, USA
| | - Taylor Rodman
- Department of Molecular Physiology and Biophysics, Vanderbilt University, Nashville, Tennessee, USA
| | - Kinuthia Kabugi
- Department of Molecular Physiology and Biophysics, Vanderbilt University, Nashville, Tennessee, USA
| | - Alice Koh
- Department of Molecular Physiology and Biophysics, Vanderbilt University, Nashville, Tennessee, USA
| | - Suzanne Navarro
- Department of Molecular Physiology and Biophysics, Vanderbilt University, Nashville, Tennessee, USA
| | - Jacob Lam
- Department of Internal Medicine, University of Iowa, Iowa City, Iowa, USA
| | - Ben Kirk
- Department of Internal Medicine, University of Iowa, Iowa City, Iowa, USA
| | - Margaret Mungai
- Department of Molecular Physiology and Biophysics, Vanderbilt University, Nashville, Tennessee, USA
- Department of Internal Medicine, University of Iowa, Iowa City, Iowa, USA
| | - Mariya Sweetwyne
- Department of Laboratory Medicine and Pathology, University of Washington, Seattle, Washington, USA
| | - Ho-Jin Koh
- Department of Biological Sciences, Tennessee State University, Nashville, Tennessee, USA
| | - Elma Zaganjor
- Department of Molecular Physiology and Biophysics, Vanderbilt University, Nashville, Tennessee, USA
| | - Steven M Damo
- Department of Life and Physical Sciences, Fisk University, Nashville, Tennessee, USA
| | - Jennifer A Gaddy
- Division of Infectious Diseases, Vanderbilt University School of Medicine, Nashville, Tennessee, USA
- Tennessee Valley Healthcare Systems, U.S. Department of Veterans Affairs, Nashville, Tennessee, USA
| | - Annet Kirabo
- Department of Medicine, Division of Clinical Pharmacology, Vanderbilt University Medical Center, Nashville, Tennessee, USA
| | - Sandra A Murray
- Department of Cell Biology, School of Medicine, University of Pittsburgh, Pittsburgh, Pennsylvania, USA
| | - Anthonya Cooper
- Department of Cell Biology, School of Medicine, University of Pittsburgh, Pittsburgh, Pennsylvania, USA
| | - Clintoria Williams
- Department of Neuroscience, Cell Biology and Physiology, Wright State University, Dayton, Ohio, USA
| | - Melanie R McReynolds
- Department of Biochemistry and Molecular Biology, Pennsylvania State University, University Park, Pennsylvania, USA
- Huck Institutes of the Life Sciences, Pennsylvania State University, University Park, Pennsylvania, USA
| | - Andrea G Marshall
- Department of Molecular Physiology and Biophysics, Vanderbilt University, Nashville, Tennessee, USA
| | - Antentor Hinton
- Department of Molecular Physiology and Biophysics, Vanderbilt University, Nashville, Tennessee, USA
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Konopová B, Týč J. Minimal resin embedding of SBF-SEM samples reduces charging and facilitates finding a surface-linked region of interest. Front Zool 2023; 20:29. [PMID: 37641135 PMCID: PMC10463905 DOI: 10.1186/s12983-023-00507-x] [Citation(s) in RCA: 0] [Impact Index Per Article: 0] [Reference Citation Analysis] [Abstract] [Key Words] [Grants] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Received: 03/06/2023] [Accepted: 08/02/2023] [Indexed: 08/31/2023] Open
Abstract
BACKGROUND For decoding the mechanism of how cells and organs function information on their ultrastructure is essential. High-resolution 3D imaging has revolutionized morphology. Serial block face scanning electron microscopy (SBF-SEM) offers non-laborious, automated imaging in 3D of up to ~ 1 mm3 large biological objects at nanometer-scale resolution. For many samples there are obstacles. Quality imaging is often hampered by charging effects, which originate in the nonconductive resin used for embedding. Especially, if the imaged region of interest (ROI) includes the surface of the sample and neighbours the empty resin, which insulates the object. This extra resin also obscures the sample's morphology, thus making navigation to the ROI difficult. RESULTS Using the example of small arthropods and a fish roe we describe a workflow to prepare samples for SBF-SEM using the minimal resin (MR) embedding method. We show that for imaging of surface structures this simple approach conveniently tackles and solves both of the two major problems-charging and ROI localization-that complicate imaging of SBF-SEM samples embedded in an excess of overlying resin. As the surface ROI is not masked by the resin, samples can be precisely trimmed before they are placed into the imaging chamber. The initial approaching step is fast and easy. No extra trimming inside the microscope is necessary. Importantly, charging is absent or greatly reduced meaning that imaging can be accomplished under good vacuum conditions, typically at the optimal high vacuum. This leads to better resolution, better signal to noise ratio, and faster image acquisition. CONCLUSIONS In MR embedded samples charging is minimized and ROI easily targeted. MR embedding does not require any special equipment or skills. It saves effort, microscope time and eventually leads to high quality data. Studies on surface-linked ROIs, or any samples normally surrounded by the excess of resin, would benefit from adopting the technique.
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Affiliation(s)
- Barbora Konopová
- Institute of Entomology, Biology Centre CAS, České Budějovice, Czech Republic.
- Department of Zoology, Faculty of Science, University of South Bohemia, České Budějovice, Czech Republic.
| | - Jiří Týč
- Institute of Parasitology, Biology Centre CAS, České Budějovice, Czech Republic.
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Koban M, Machálková M, Javůrek J. An Integrated Solution for the Complete Serial Block-Face Scanning Electron Microscopy Workflow: From Image Acquisition to Data Processing. MICROSCOPY AND MICROANALYSIS : THE OFFICIAL JOURNAL OF MICROSCOPY SOCIETY OF AMERICA, MICROBEAM ANALYSIS SOCIETY, MICROSCOPICAL SOCIETY OF CANADA 2023; 29:1213-1215. [PMID: 37613333 DOI: 10.1093/micmic/ozad067.624] [Citation(s) in RCA: 0] [Impact Index Per Article: 0] [Reference Citation Analysis] [Track Full Text] [Subscribe] [Scholar Register] [Indexed: 08/25/2023]
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4
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Collinson LM, Bosch C, Bullen A, Burden JJ, Carzaniga R, Cheng C, Darrow MC, Fletcher G, Johnson E, Narayan K, Peddie CJ, Winn M, Wood C, Patwardhan A, Kleywegt GJ, Verkade P. Volume EM: a quiet revolution takes shape. Nat Methods 2023; 20:777-782. [PMID: 37076630 PMCID: PMC7614633 DOI: 10.1038/s41592-023-01861-8] [Citation(s) in RCA: 18] [Impact Index Per Article: 18.0] [Reference Citation Analysis] [Abstract] [MESH Headings] [Grants] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Indexed: 04/21/2023]
Abstract
Volume Electron Microscopy is a group of techniques that reveal the 3D ultrastructure of cells and tissues through volumes greater than 1 cubic micron. A burgeoning grass roots community effort is fast building the profile, and revealing the impact, of vEM technology in the life sciences and clinical research.
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Affiliation(s)
- Lucy M Collinson
- Electron Microscopy Science Technology Platform, Francis Crick Institute, London, UK.
| | - Carles Bosch
- Sensory Circuits and Neurotechnology Laboratory, Francis Crick Institute, London, UK
| | - Anwen Bullen
- UCL Ear Institute, University College London, London, UK
| | - Jemima J Burden
- Laboratory for Molecular Cell Biology, University College London, London, UK
| | - Raffaella Carzaniga
- Zeiss Research Microscopy Solutions, Carl Zeiss Ltd, Zeiss Group, Cambourne, UK
| | | | - Michele C Darrow
- Artificial Intelligence & Informatics, The Rosalind Franklin Institute, Didcot, UK
- SPT Labtech Ltd., Melbourn, UK
| | | | - Errin Johnson
- Dunn School Bioimaging Facility, Sir William Dunn School of Pathology, Oxford University, Oxford, UK
| | - Kedar Narayan
- Center for Molecular Microscopy, Center for Cancer Research, National Cancer Institute, National Institutes of Health, Bethesda, MD, USA
- Cancer Research Technology Program, Frederick National Laboratory for Cancer Research, Frederick, MD, USA
| | - Christopher J Peddie
- Electron Microscopy Science Technology Platform, Francis Crick Institute, London, UK
| | - Martyn Winn
- UKRI-STFC, Rutherford Appleton Laboratory, Didcot, UK
| | - Charles Wood
- Future Technology Centre, School of Mechanical and Design Engineering, University of Portsmouth, Portsmouth, UK
| | - Ardan Patwardhan
- European Molecular Biology Laboratory, European Bioinformatics Institute (EMBL-EBI), Hinxton, UK
| | - Gerard J Kleywegt
- European Molecular Biology Laboratory, European Bioinformatics Institute (EMBL-EBI), Hinxton, UK
| | - Paul Verkade
- School of Biochemistry, University of Bristol, Bristol, UK.
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Stempinski ES, Pagano L, Riesterer JL, Adamou SK, Thibault G, Song X, Chang YH, López CS. Automated large volume sample preparation for vEM. Methods Cell Biol 2023; 177:1-32. [PMID: 37451763 DOI: 10.1016/bs.mcb.2023.01.009] [Citation(s) in RCA: 1] [Impact Index Per Article: 1.0] [Reference Citation Analysis] [Abstract] [Key Words] [MESH Headings] [Grants] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Indexed: 07/18/2023]
Abstract
New developments in electron microscopy technology, improved efficiency of detectors, and artificial intelligence applications for data analysis over the past decade have increased the use of volume electron microscopy (vEM) in the life sciences field. Moreover, sample preparation methods are continuously being modified by investigators to improve final sample quality, increase electron density, combine imaging technologies, and minimize the introduction of artifacts into specimens under study. There are a variety of conventional bench protocols that a researcher can utilize, though most of these protocols require several days. In this work, we describe the utilization of an automated specimen processor, the mPrep™ ASP-2000™, to prepare samples for vEM that are compatible with focused ion beam scanning electron microscopy (FIB-SEM), serial block face scanning electron microscopy (SBF-SEM), and array tomography (AT). The protocols described here aimed for methods that are completed in a much shorter period of time while minimizing the exposure of the operator to hazardous and toxic chemicals and improving the reproducibility of the specimens' heavy metal staining, all without compromising the quality of the data acquired using backscattered electrons during SEM imaging. As a control, we have included a widely used sample bench protocol and have utilized it as a comparator for image quality analysis, both qualitatively and using image quality analysis metrics.
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Affiliation(s)
- Erin S Stempinski
- Multiscale Microscopy Core, Oregon Health & Science University, Portland, OR, United States
| | - Lucas Pagano
- Knight Cancer Institute-CEDAR, Oregan Health & Science University, Portland, OR, United States
| | - Jessica L Riesterer
- Multiscale Microscopy Core, Oregon Health & Science University, Portland, OR, United States; Knight Cancer Institute-CEDAR, Oregan Health & Science University, Portland, OR, United States
| | - Steven K Adamou
- Multiscale Microscopy Core, Oregon Health & Science University, Portland, OR, United States
| | - Guillaume Thibault
- Knight Cancer Institute-CEDAR, Oregan Health & Science University, Portland, OR, United States; Department of Biomedical Engineering, Oregon Health & Science University, Portland, OR, United States
| | - Xubo Song
- Knight Cancer Institute-CEDAR, Oregan Health & Science University, Portland, OR, United States
| | - Young Hwan Chang
- Department of Biomedical Engineering, Oregon Health & Science University, Portland, OR, United States
| | - Claudia S López
- Multiscale Microscopy Core, Oregon Health & Science University, Portland, OR, United States; Department of Biomedical Engineering, Oregon Health & Science University, Portland, OR, United States; Pacific Northwest Center for Cryo-EM, Oregon Health & Science University, Portland, OR, United States.
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6
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Borghgraef P, Kremer A, De Bruyne M, Guérin CJ, Lippens S. Resin comparison for serial block face scanning volume electron microscopy. Methods Cell Biol 2023; 177:33-54. [PMID: 37451773 DOI: 10.1016/bs.mcb.2023.01.011] [Citation(s) in RCA: 0] [Impact Index Per Article: 0] [Reference Citation Analysis] [Abstract] [Key Words] [MESH Headings] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Indexed: 03/14/2023]
Abstract
Serial Block Face Scanning Electron Microscopy (SBF-SEM) is one of several volume electron microscopy (vEM) techniques whose purpose is to reveal the nanostructure of cells and tissues in three dimensions. As one of the earliest, and possibly most widely adopted of the disruptive vEM techniques there have been hundreds of publications using the method, although very few comparative studies of specimen preparation parameters. While some studies have focused on staining and specimen acquisition no comparison of resin embedding has yet been conducted. To this end we have surveyed the SBF-SEM literature to determine which resins are commonly used and compared them in both cellular and fixed tissue samples in an attempt to optimize sample preparation for: effectiveness of resin infiltration, resistance to charging and beam damage and clarity of image in the resulting data set. Here we present the results and discuss the various factors that go into optimizing specimen preparation for SBF-SEM.
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Affiliation(s)
- Peter Borghgraef
- VIB Bioimaging Core, VIB, Ghent, Belgium; VIB-UGent Center for Inflammation Research, VIB, Ghent, Belgium; Department of Biomedical Molecular Biology, Ghent University, Ghent, Belgium
| | - Anna Kremer
- VIB Bioimaging Core, VIB, Ghent, Belgium; VIB-UGent Center for Inflammation Research, VIB, Ghent, Belgium; Department of Biomedical Molecular Biology, Ghent University, Ghent, Belgium
| | - Michiel De Bruyne
- VIB Bioimaging Core, VIB, Ghent, Belgium; VIB-UGent Center for Inflammation Research, VIB, Ghent, Belgium; Department of Biomedical Molecular Biology, Ghent University, Ghent, Belgium
| | - Christopher J Guérin
- VIB Bioimaging Core, VIB, Ghent, Belgium; VIB-UGent Center for Inflammation Research, VIB, Ghent, Belgium; Department of Biomedical Molecular Biology, Ghent University, Ghent, Belgium
| | - Saskia Lippens
- VIB Bioimaging Core, VIB, Ghent, Belgium; VIB-UGent Center for Inflammation Research, VIB, Ghent, Belgium; Department of Biomedical Molecular Biology, Ghent University, Ghent, Belgium.
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7
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Raimondi A, Ilacqua N, Pellegrini L. Liver inter-organelle membrane contact sites revealed by serial section electron tomography. Methods Cell Biol 2023; 177:101-123. [PMID: 37451764 DOI: 10.1016/bs.mcb.2022.12.021] [Citation(s) in RCA: 0] [Impact Index Per Article: 0] [Reference Citation Analysis] [Abstract] [Key Words] [MESH Headings] [Grants] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Indexed: 02/12/2023]
Abstract
Inter-organelle membrane contact sites (MCSs) are defined as areas of close proximity between the membranes of two organelles (10-80nm). They have been implicated in many physiological processes such as Ca++, lipids or small molecules transfer, organelles biogenesis or dynamic and have an important role in many cellular processes such as apoptosis, autophagy, and signaling. Since the distance and the extent of these contacts are in the nanometer range, high resolution techniques are ideal for imaging these structures. It is for this reason that transmission electron microscopy (TEM) has been considered the gold standard for MCSs visualization and the first technique that described them. However, often TEM analysis is limited to 2D lacking information on the 3D association between the organelles involved in MCSs. To fully describe the complex architecture of MSCs and to unveil their role in cellular physiology a 3D analysis is required. This chapter provides a method for the analysis of MCSs using serial section electron tomography (ssET), a technique able to reconstruct in 3D at nanometer resolution cellular and subcellular structures. By applying this procedure, it was possible to elucidate the role of the contacts between Endoplasmic Reticulum (ER) and other organelles in liver lipid metabolism.
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Affiliation(s)
- Andrea Raimondi
- Experimental Imaging Centre, IRCCS San Raffaele Scientific Institute, Milan, Italy.
| | - Nicolò Ilacqua
- Mitochondria Biology Laboratory, Brain Research Center, Quebec, QC, Canada; Department of Molecular Biology, Medical Biochemistry and Pathology, Faculty of Medicine, Laval University, Quebec, QC, Canada
| | - Luca Pellegrini
- Mitochondria Biology Laboratory, Brain Research Center, Quebec, QC, Canada; Department of Molecular Biology, Medical Biochemistry and Pathology, Faculty of Medicine, Laval University, Quebec, QC, Canada; Department of Biochemistry, Microbiology and Immunology, Faculty of Medicine, University of Ottawa, Ottawa, ON, Canada.
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8
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Bélanger S, Berensmann H, Baena V, Duncan K, Meyers BC, Narayan K, Czymmek KJ. A versatile enhanced freeze-substitution protocol for volume electron microscopy. Front Cell Dev Biol 2022; 10:933376. [PMID: 36003147 PMCID: PMC9393620 DOI: 10.3389/fcell.2022.933376] [Citation(s) in RCA: 0] [Impact Index Per Article: 0] [Reference Citation Analysis] [Abstract] [Track Full Text] [Download PDF] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Received: 04/30/2022] [Accepted: 07/08/2022] [Indexed: 11/18/2022] Open
Abstract
Volume electron microscopy, a powerful approach to generate large three-dimensional cell and tissue volumes at electron microscopy resolutions, is rapidly becoming a routine tool for understanding fundamental and applied biological questions. One of the enabling factors for its adoption has been the development of conventional fixation protocols with improved heavy metal staining. However, freeze-substitution with organic solvent-based fixation and staining has not realized the same level of benefit. Here, we report a straightforward approach including osmium tetroxide, acetone and up to 3% water substitution fluid (compatible with traditional or fast freeze-substitution protocols), warm-up and transition from organic solvent to aqueous 2% osmium tetroxide. Once fully hydrated, samples were processed in aqueous based potassium ferrocyanide, thiocarbohydrazide, osmium tetroxide, uranyl acetate and lead acetate before resin infiltration and polymerization. We observed a consistent and substantial increase in heavy metal staining across diverse and difficult-to-fix test organisms and tissue types, including plant tissues (Hordeum vulgare), nematode (Caenorhabditis elegans) and yeast (Saccharomyces cerevisiae). Our approach opens new possibilities to combine the benefits of cryo-preservation with enhanced contrast for volume electron microscopy in diverse organisms.
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Affiliation(s)
| | - Heather Berensmann
- Center for Molecular Microscopy, Center for Cancer Research, National Cancer Institute, National Institutes of Health, Bethesda, MD, United States
- Cancer Research Technology Program, Frederick National Laboratory for Cancer Research, Frederick, MD, United States
| | - Valentina Baena
- Center for Molecular Microscopy, Center for Cancer Research, National Cancer Institute, National Institutes of Health, Bethesda, MD, United States
- Cancer Research Technology Program, Frederick National Laboratory for Cancer Research, Frederick, MD, United States
| | - Keith Duncan
- Donald Danforth Plant Science Center, Saint Louis, MO, United States
| | - Blake C. Meyers
- Donald Danforth Plant Science Center, Saint Louis, MO, United States
- Division of Plant Science and Technology, University of Missouri–Columbia, Columbia, MO, United States
| | - Kedar Narayan
- Center for Molecular Microscopy, Center for Cancer Research, National Cancer Institute, National Institutes of Health, Bethesda, MD, United States
- Cancer Research Technology Program, Frederick National Laboratory for Cancer Research, Frederick, MD, United States
| | - Kirk J. Czymmek
- Donald Danforth Plant Science Center, Saint Louis, MO, United States
- Advanced Bioimaging Laboratory, Donald Danforth Plant Science Center, Saint Louis, MO, United States
- *Correspondence: Kirk J. Czymmek,
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9
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Peddie CJ, Genoud C, Kreshuk A, Meechan K, Micheva KD, Narayan K, Pape C, Parton RG, Schieber NL, Schwab Y, Titze B, Verkade P, Aubrey A, Collinson LM. Volume electron microscopy. NATURE REVIEWS. METHODS PRIMERS 2022; 2:51. [PMID: 37409324 PMCID: PMC7614724 DOI: 10.1038/s43586-022-00131-9] [Citation(s) in RCA: 35] [Impact Index Per Article: 17.5] [Reference Citation Analysis] [Abstract] [Track Full Text] [Subscribe] [Scholar Register] [Accepted: 05/10/2022] [Indexed: 07/07/2023]
Abstract
Life exists in three dimensions, but until the turn of the century most electron microscopy methods provided only 2D image data. Recently, electron microscopy techniques capable of delving deep into the structure of cells and tissues have emerged, collectively called volume electron microscopy (vEM). Developments in vEM have been dubbed a quiet revolution as the field evolved from established transmission and scanning electron microscopy techniques, so early publications largely focused on the bioscience applications rather than the underlying technological breakthroughs. However, with an explosion in the uptake of vEM across the biosciences and fast-paced advances in volume, resolution, throughput and ease of use, it is timely to introduce the field to new audiences. In this Primer, we introduce the different vEM imaging modalities, the specialized sample processing and image analysis pipelines that accompany each modality and the types of information revealed in the data. We showcase key applications in the biosciences where vEM has helped make breakthrough discoveries and consider limitations and future directions. We aim to show new users how vEM can support discovery science in their own research fields and inspire broader uptake of the technology, finally allowing its full adoption into mainstream biological imaging.
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Affiliation(s)
- Christopher J. Peddie
- Electron Microscopy Science Technology Platform, The Francis Crick Institute, London, UK
| | - Christel Genoud
- Electron Microscopy Facility, Faculty of Biology and Medicine, University of Lausanne, Lausanne, Switzerland
| | - Anna Kreshuk
- Cell Biology and Biophysics Unit, European Molecular Biology Laboratory, Heidelberg, Germany
| | - Kimberly Meechan
- Cell Biology and Biophysics Unit, European Molecular Biology Laboratory, Heidelberg, Germany
- Present address: Faculty of Biosciences, Heidelberg University, Heidelberg, Germany
| | - Kristina D. Micheva
- Department of Molecular and Cellular Physiology, Stanford University, Palo Alto, CA, USA
| | - Kedar Narayan
- Center for Molecular Microscopy, Center for Cancer Research, National Cancer Institute, National Institutes of Health, Bethesda, MD, USA
- Cancer Research Technology Program, Frederick National Laboratory for Cancer Research, Frederick, MD, USA
| | - Constantin Pape
- Cell Biology and Biophysics Unit, European Molecular Biology Laboratory, Heidelberg, Germany
| | - Robert G. Parton
- The Institute for Molecular Bioscience, The University of Queensland, Brisbane, Queensland, Australia
- Centre for Microscopy and Microanalysis, The University of Queensland, Brisbane, Queensland, Australia
| | - Nicole L. Schieber
- Centre for Microscopy and Microanalysis, The University of Queensland, Brisbane, Queensland, Australia
| | - Yannick Schwab
- Cell Biology and Biophysics Unit/ Electron Microscopy Core Facility, European Molecular Biology Laboratory, Heidelberg, Germany
| | | | - Paul Verkade
- School of Biochemistry, University of Bristol, Bristol, UK
| | - Aubrey Aubrey
- Janelia Research Campus, Howard Hughes Medical Institute, Ashburn, VA, USA
| | - Lucy M. Collinson
- Electron Microscopy Science Technology Platform, The Francis Crick Institute, London, UK
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10
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Brenna C, Simioni C, Varano G, Conti I, Costanzi E, Melloni M, Neri LM. Optical tissue clearing associated with 3D imaging: application in preclinical and clinical studies. Histochem Cell Biol 2022; 157:497-511. [PMID: 35235045 PMCID: PMC9114043 DOI: 10.1007/s00418-022-02081-5] [Citation(s) in RCA: 6] [Impact Index Per Article: 3.0] [Reference Citation Analysis] [Abstract] [Key Words] [Track Full Text] [Download PDF] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Accepted: 01/28/2022] [Indexed: 12/23/2022]
Abstract
Understanding the inner morphology of intact tissues is one of the most competitive challenges in modern biology. Since the beginning of the twentieth century, optical tissue clearing (OTC) has provided solutions for volumetric imaging, allowing the microscopic visualization of thick sections of tissue, organoids, up to whole organs and organisms (for example, mouse or rat). Recently, tissue clearing has also been introduced in clinical settings to achieve a more accurate diagnosis with the support of 3D imaging. This review aims to give an overview of the most recent developments in OTC and 3D imaging and to illustrate their role in the field of medical diagnosis, with a specific focus on clinical applications.
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Affiliation(s)
- Cinzia Brenna
- Department of Translational Medicine, University of Ferrara, 44121, Ferrara, Italy.,Medical Research Center, Medical Faculty Mannheim, University of Heidelberg, Theodor-Kutzer-Ufer 1-3, 68167, Mannheim, Germany
| | - Carolina Simioni
- Department of Life Sciences and Biotechnology, University of Ferrara, 44121, Ferrara, Italy.,LTTA - Electron Microscopy Center, University of Ferrara, 44121, Ferrara, Italy
| | - Gabriele Varano
- Department of Translational Medicine, University of Ferrara, 44121, Ferrara, Italy
| | - Ilaria Conti
- Department of Translational Medicine, University of Ferrara, 44121, Ferrara, Italy
| | - Eva Costanzi
- Department of Translational Medicine, University of Ferrara, 44121, Ferrara, Italy
| | - Mattia Melloni
- Department of Translational Medicine, University of Ferrara, 44121, Ferrara, Italy
| | - Luca Maria Neri
- Department of Translational Medicine, University of Ferrara, 44121, Ferrara, Italy. .,LTTA - Electron Microscopy Center, University of Ferrara, 44121, Ferrara, Italy.
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Garza-Lopez E, Vue Z, Katti P, Neikirk K, Biete M, Lam J, Beasley HK, Marshall AG, Rodman TA, Christensen TA, Salisbury JL, Vang L, Mungai M, AshShareef S, Murray SA, Shao J, Streeter J, Glancy B, Pereira RO, Abel ED, Hinton A. Protocols for Generating Surfaces and Measuring 3D Organelle Morphology Using Amira. Cells 2021; 11:65. [PMID: 35011629 PMCID: PMC8750564 DOI: 10.3390/cells11010065] [Citation(s) in RCA: 36] [Impact Index Per Article: 12.0] [Reference Citation Analysis] [Abstract] [Key Words] [MESH Headings] [Grants] [Track Full Text] [Download PDF] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Received: 09/25/2021] [Revised: 12/18/2021] [Accepted: 12/22/2021] [Indexed: 12/14/2022] Open
Abstract
High-resolution 3D images of organelles are of paramount importance in cellular biology. Although light microscopy and transmission electron microscopy (TEM) have provided the standard for imaging cellular structures, they cannot provide 3D images. However, recent technological advances such as serial block-face scanning electron microscopy (SBF-SEM) and focused ion beam scanning electron microscopy (FIB-SEM) provide the tools to create 3D images for the ultrastructural analysis of organelles. Here, we describe a standardized protocol using the visualization software, Amira, to quantify organelle morphologies in 3D, thereby providing accurate and reproducible measurements of these cellular substructures. We demonstrate applications of SBF-SEM and Amira to quantify mitochondria and endoplasmic reticulum (ER) structures.
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Affiliation(s)
- Edgar Garza-Lopez
- Hinton and Garza Lopez Family Consulting Company, Iowa City, IA 52246, USA;
| | - Zer Vue
- Department of Molecular Physiology and Biophysics, Vanderbilt University, Nashville, TN 37232, USA; (Z.V.); (H.K.B.); (A.G.M.); (T.A.R.); (L.V.)
| | - Prasanna Katti
- National Heart, Lung, and Blood Institute, National Institutes of Health, Bethesda, MD 20892, USA; (P.K.); (B.G.)
| | - Kit Neikirk
- Department of Biology, University of Hawaii at Hilo, Hilo, HI 96720, USA; (K.N.); (M.B.)
| | - Michelle Biete
- Department of Biology, University of Hawaii at Hilo, Hilo, HI 96720, USA; (K.N.); (M.B.)
| | - Jacob Lam
- Department of Internal Medicine, Carver College of Medicine, University of Iowa, Iowa City, IA 52242, USA; (J.L.); (M.M.); (S.A.); (J.S.)
| | - Heather K. Beasley
- Department of Molecular Physiology and Biophysics, Vanderbilt University, Nashville, TN 37232, USA; (Z.V.); (H.K.B.); (A.G.M.); (T.A.R.); (L.V.)
- Department of Biochemistry, Cancer Biology, Neuroscience and Pharmacology, School of Graduate Studies and Research, Meharry Medical College, Nashville, TN 37208, USA
| | - Andrea G. Marshall
- Department of Molecular Physiology and Biophysics, Vanderbilt University, Nashville, TN 37232, USA; (Z.V.); (H.K.B.); (A.G.M.); (T.A.R.); (L.V.)
| | - Taylor A. Rodman
- Department of Molecular Physiology and Biophysics, Vanderbilt University, Nashville, TN 37232, USA; (Z.V.); (H.K.B.); (A.G.M.); (T.A.R.); (L.V.)
| | - Trace A. Christensen
- Microscopy and Cell Analysis Core Facility, Mayo Clinic, Rochester, MN 55905, USA; (T.A.C.); (J.L.S.)
| | - Jeffrey L. Salisbury
- Microscopy and Cell Analysis Core Facility, Mayo Clinic, Rochester, MN 55905, USA; (T.A.C.); (J.L.S.)
- Department of Biochemistry and Molecular Biology, Mayo Clinic, Rochester, MN 55905, USA
| | - Larry Vang
- Department of Molecular Physiology and Biophysics, Vanderbilt University, Nashville, TN 37232, USA; (Z.V.); (H.K.B.); (A.G.M.); (T.A.R.); (L.V.)
| | - Margaret Mungai
- Department of Internal Medicine, Carver College of Medicine, University of Iowa, Iowa City, IA 52242, USA; (J.L.); (M.M.); (S.A.); (J.S.)
| | - Salma AshShareef
- Department of Internal Medicine, Carver College of Medicine, University of Iowa, Iowa City, IA 52242, USA; (J.L.); (M.M.); (S.A.); (J.S.)
| | - Sandra A. Murray
- Department of Cell Biology, School of Medicine, University of Pittsburgh, Pittsburgh, PA 52013, USA;
| | - Jianqiang Shao
- Central Microscopy Research Facility, University of Iowa, Iowa City, IA 52242, USA;
| | - Jennifer Streeter
- Department of Internal Medicine, Carver College of Medicine, University of Iowa, Iowa City, IA 52242, USA; (J.L.); (M.M.); (S.A.); (J.S.)
- Fraternal Order of Eagles Diabetes Research Center, Iowa City, IA 52242, USA
| | - Brian Glancy
- National Heart, Lung, and Blood Institute, National Institutes of Health, Bethesda, MD 20892, USA; (P.K.); (B.G.)
| | - Renata O. Pereira
- Department of Internal Medicine, Carver College of Medicine, University of Iowa, Iowa City, IA 52242, USA; (J.L.); (M.M.); (S.A.); (J.S.)
- Fraternal Order of Eagles Diabetes Research Center, Iowa City, IA 52242, USA
| | - E. Dale Abel
- Department of Internal Medicine, Carver College of Medicine, University of Iowa, Iowa City, IA 52242, USA; (J.L.); (M.M.); (S.A.); (J.S.)
- Fraternal Order of Eagles Diabetes Research Center, Iowa City, IA 52242, USA
| | - Antentor Hinton
- Hinton and Garza Lopez Family Consulting Company, Iowa City, IA 52246, USA;
- Department of Molecular Physiology and Biophysics, Vanderbilt University, Nashville, TN 37232, USA; (Z.V.); (H.K.B.); (A.G.M.); (T.A.R.); (L.V.)
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12
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Lewczuk B, Szyryńska N. Field-Emission Scanning Electron Microscope as a Tool for Large-Area and Large-Volume Ultrastructural Studies. Animals (Basel) 2021; 11:ani11123390. [PMID: 34944167 PMCID: PMC8698110 DOI: 10.3390/ani11123390] [Citation(s) in RCA: 2] [Impact Index Per Article: 0.7] [Reference Citation Analysis] [Abstract] [Key Words] [Track Full Text] [Download PDF] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Received: 10/31/2021] [Revised: 11/24/2021] [Accepted: 11/25/2021] [Indexed: 11/29/2022] Open
Abstract
Simple Summary Ultrastructural studies of cells and tissues are usually performed using transmission electron microscopy (TEM), which enables imaging at the highest possible resolution. The weak point of TEM is the limited ability to analyze the ultrastructure of large areas and volumes of biological samples. This limitation can be overcome by using modern field-emission scanning electron microscopy (FE-SEM) with high-sensitivity detection, which enables the creation of TEM-like images from the flat surfaces of resin-embedded biological specimens. Several FE-SEM-based techniques for two- and three-dimensional ultrastructural studies of cells, tissues, organs, and organisms have been developed in the 21st century. These techniques have created a new era in structural biology and have changed the role of the scanning electron microscope (SEM) in biological and medical laboratories. Since the premiere of the first commercially available SEM in 1965, these instruments were used almost exclusively to obtain topographical information over a large range of magnifications. Currently, FE-SEM offers many attractive possibilities in the studies of cell and tissue ultrastructure, and they are presented in this review. Abstract The development of field-emission scanning electron microscopes for high-resolution imaging at very low acceleration voltages and equipped with highly sensitive detectors of backscattered electrons (BSE) has enabled transmission electron microscopy (TEM)-like imaging of the cut surfaces of tissue blocks, which are impermeable to the electron beam, or tissue sections mounted on the solid substrates. This has resulted in the development of methods that simplify and accelerate ultrastructural studies of large areas and volumes of biological samples. This article provides an overview of these methods, including their advantages and disadvantages. The imaging of large sample areas can be performed using two methods based on the detection of transmitted electrons or BSE. Effective imaging using BSE requires special fixation and en bloc contrasting of samples. BSE imaging has resulted in the development of volume imaging techniques, including array tomography (AT) and serial block-face imaging (SBF-SEM). In AT, serial ultrathin sections are collected manually on a solid substrate such as a glass and silicon wafer or automatically on a tape using a special ultramicrotome. The imaging of serial sections is used to obtain three-dimensional (3D) information. SBF-SEM is based on removing the top layer of a resin-embedded sample using an ultramicrotome inside the SEM specimen chamber and then imaging the exposed surface with a BSE detector. The steps of cutting and imaging the resin block are repeated hundreds or thousands of times to obtain a z-stack for 3D analyses.
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13
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Ashaber M, Tomina Y, Kassraian P, Bushong EA, Kristan WB, Ellisman MH, Wagenaar DA. Anatomy and activity patterns in a multifunctional motor neuron and its surrounding circuits. eLife 2021; 10:e61881. [PMID: 33587033 PMCID: PMC7954528 DOI: 10.7554/elife.61881] [Citation(s) in RCA: 2] [Impact Index Per Article: 0.7] [Reference Citation Analysis] [Abstract] [Key Words] [MESH Headings] [Grants] [Track Full Text] [Download PDF] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Received: 08/07/2020] [Accepted: 02/12/2021] [Indexed: 12/27/2022] Open
Abstract
Dorsal Excitor motor neuron DE-3 in the medicinal leech plays three very different dynamical roles in three different behaviors. Without rewiring its anatomical connectivity, how can a motor neuron dynamically switch roles to play appropriate roles in various behaviors? We previously used voltage-sensitive dye imaging to record from DE-3 and most other neurons in the leech segmental ganglion during (fictive) swimming, crawling, and local-bend escape (Tomina and Wagenaar, 2017). Here, we repeated that experiment, then re-imaged the same ganglion using serial blockface electron microscopy and traced DE-3's processes. Further, we traced back the processes of DE-3's presynaptic partners to their respective somata. This allowed us to analyze the relationship between circuit anatomy and the activity patterns it sustains. We found that input synapses important for all the behaviors were widely distributed over DE-3's branches, yet that functional clusters were different during (fictive) swimming vs. crawling.
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Affiliation(s)
- Mária Ashaber
- Division of Biology and Biological Engineering, California Institute of TechnologyPasadenaUnited States
| | - Yusuke Tomina
- Division of Biology and Biological Engineering, California Institute of TechnologyPasadenaUnited States
| | - Pegah Kassraian
- Division of Biology and Biological Engineering, California Institute of TechnologyPasadenaUnited States
| | - Eric A Bushong
- Division of Biological Sciences, University of California, San DiegoSan DiegoUnited States
| | - William B Kristan
- Division of Biological Sciences, University of California, San DiegoSan DiegoUnited States
| | - Mark H Ellisman
- National Center for Microscopy and Imaging Research, University of California, San DiegoSan DiegoUnited States
- Department of Neurosciences, UCSD School of MedicineSan DiegoUnited States
| | - Daniel A Wagenaar
- Division of Biology and Biological Engineering, California Institute of TechnologyPasadenaUnited States
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14
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Xu X, Zhu L, Xue K, Liu J, Wang J, Wang G, Gu J, Zhang Y, Li X. Ultrastructural studies of the neurovascular unit reveal enhanced endothelial transcytosis in hyperglycemia‐enhanced hemorrhagic transformation after stroke. CNS Neurosci Ther 2021. [PMCID: PMC7804894 DOI: 10.1111/cns.13571] [Citation(s) in RCA: 4] [Impact Index Per Article: 1.3] [Reference Citation Analysis] [Abstract] [Track Full Text] [Download PDF] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Indexed: 12/12/2022] Open
Abstract
Aims Pre‐existing hyperglycemia (HG) aggravates the breakdown of blood–brain barrier (BBB) and increases the risk of hemorrhagic transformation (HT) after acute ischemic stroke in both animal models and patients. To date, HG‐induced ultrastructural changes of brain microvascular endothelial cells (BMECs) and the mechanisms underlying HG‐enhanced HT after ischemic stroke are poorly understood. Methods We used a mouse model of mild brain ischemia/reperfusion to investigate HG‐induced ultrastructural changes of BMECs that contribute to the impairment of BBB integrity after stroke. Adult male mice received systemic glucose administration 15 min before middle cerebral artery occlusion (MCAO) for 20 min. Ultrastructural characteristics of BMECs were evaluated using two‐dimensional and three‐dimensional electron microscopy and quantitatively analyzed. Results Mice with acute HG had exacerbated BBB disruption and larger brain infarcts compared to mice with normoglycemia (NG) after MCAO and 4 h of reperfusion, as assessed by brain extravasation of the Evans blue dye and microtubule‐associated protein 2 immunostaining. Electron microscopy further revealed that HG mice had more endothelial vesicles in the striatal neurovascular unit than NG mice, which may account for their deterioration of BBB impairment. In contrast with enhanced endothelial transcytosis, paracellular tight junction ultrastructure was not disrupted after this mild ischemia/reperfusion insult or altered upon HG. Consistent with the observed increase of endothelial vesicles, transcytosis‐related proteins caveolin‐1, clathrin, and hypoxia‐inducible factor (HIF)‐1α were upregulated by HG after MCAO and reperfusion. Conclusion Our study provides solid structural evidence to understand the role of endothelial transcytosis in HG‐elicited BBB hyperpermeability. Enhanced transcytosis occurs prior to the physical breakdown of BMECs and is a promising therapeutic target to preserve BBB integrity.
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Affiliation(s)
- Xiaomin Xu
- Institute of Special Environmental Medicine and Department of Neurology of Affiliated Hospital Co‐innovation Center of Neuroregeneration Nantong University Nantong China
- Qidong Women's and Children's Health Qidong China
| | - Liuqi Zhu
- Institute of Special Environmental Medicine and Department of Neurology of Affiliated Hospital Co‐innovation Center of Neuroregeneration Nantong University Nantong China
| | - Ke Xue
- Institute of Special Environmental Medicine and Department of Neurology of Affiliated Hospital Co‐innovation Center of Neuroregeneration Nantong University Nantong China
| | - Jiayi Liu
- Institute of Special Environmental Medicine and Department of Neurology of Affiliated Hospital Co‐innovation Center of Neuroregeneration Nantong University Nantong China
| | - Jian Wang
- Institute of Special Environmental Medicine and Department of Neurology of Affiliated Hospital Co‐innovation Center of Neuroregeneration Nantong University Nantong China
| | - Guohua Wang
- Institute of Special Environmental Medicine and Department of Neurology of Affiliated Hospital Co‐innovation Center of Neuroregeneration Nantong University Nantong China
| | - Jin‐hua Gu
- Institute of Special Environmental Medicine and Department of Neurology of Affiliated Hospital Co‐innovation Center of Neuroregeneration Nantong University Nantong China
| | - Yunfeng Zhang
- Institute of Special Environmental Medicine and Department of Neurology of Affiliated Hospital Co‐innovation Center of Neuroregeneration Nantong University Nantong China
| | - Xia Li
- Institute of Special Environmental Medicine and Department of Neurology of Affiliated Hospital Co‐innovation Center of Neuroregeneration Nantong University Nantong China
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15
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Raeisossadati R, Ferrari MFR. Mitochondria-ER Tethering in Neurodegenerative Diseases. Cell Mol Neurobiol 2020; 42:917-930. [PMID: 33196974 DOI: 10.1007/s10571-020-01008-9] [Citation(s) in RCA: 10] [Impact Index Per Article: 2.5] [Reference Citation Analysis] [Abstract] [Key Words] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Received: 08/22/2020] [Accepted: 11/11/2020] [Indexed: 12/12/2022]
Abstract
Organelles juxtaposition has been detected for decades, although only recently gained importance due to a pivotal role in the regulation of cellular processes dependent on membrane contact sites. Endoplasmic reticulum (ER) and mitochondria interaction is a prime example of organelles contact sites. Mitochondria-associated membranes (MAM) are proposed to harbor ER-mitochondria tether complexes, mainly when these organelles are less than 30 nm apart. Dysfunctions of proteins located at the MAM are associated with neurodegenerative diseases such as Parkinson's, Alzheimer's and amyotrophic lateral sclerosis, as well as neurodevelopmental disorders; hence any malfunction in MAM can potentially trigger cell death. This review will focus on the role of ER-mitochondria contact sites, regarding calcium homeostasis, lipid metabolism, autophagy, morphology and dynamics of mitochondria, mainly in the context of neurodegenerative diseases. Approaches that have been employed so far to study organelles contact sites, as well as methods that were not used in neurosciences yet, but are promising and accurate ways to unveil the functions of MAM during neurodegeneration, is also discussed in the present review.
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Affiliation(s)
- Reza Raeisossadati
- Departamento de Genetica e Biologia Evolutiva, Instituto de Biociencias, Universidade de Sao Paulo, Sao Paulo, SP, Brazil.
| | - Merari F R Ferrari
- Departamento de Genetica e Biologia Evolutiva, Instituto de Biociencias, Universidade de Sao Paulo, Sao Paulo, SP, Brazil.
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16
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Kremer A, VAN Hamme E, Bonnardel J, Borghgraef P, GuÉrin CJ, Guilliams M, Lippens S. A workflow for 3D-CLEM investigating liver tissue. J Microsc 2020; 281:231-242. [PMID: 33034376 DOI: 10.1111/jmi.12967] [Citation(s) in RCA: 4] [Impact Index Per Article: 1.0] [Reference Citation Analysis] [Abstract] [Key Words] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Received: 07/06/2020] [Revised: 09/22/2020] [Accepted: 10/07/2020] [Indexed: 12/31/2022]
Abstract
Correlative light and electron microscopy (CLEM) is a method used to investigate the exact same region in both light and electron microscopy (EM) in order to add ultrastructural information to a light microscopic (usually fluorescent) signal. Workflows combining optical or fluorescent data with electron microscopic images are complex, hence there is a need to communicate detailed protocols and share tips & tricks for successful application of these methods. With the development of volume-EM techniques such as serial blockface scanning electron microscopy (SBF-SEM) and Focussed Ion Beam-SEM, correlation in three dimensions has become more efficient. Volume electron microscopy allows automated acquisition of serial section imaging data that can be reconstructed in three dimensions (3D) to provide a detailed, geometrically accurate view of cellular ultrastructure. In addition, combining volume-EM with high-resolution light microscopy (LM) techniques decreases the resolution gap between LM and EM, making retracing of a region of interest and eventual overlays more straightforward. Here, we present a workflow for 3D CLEM on mouse liver, combining high-resolution confocal microscopy with SBF-SEM. In this workflow, we have made use of two types of landmarks: (1) near infrared laser branding marks to find back the region imaged in LM in the electron microscope and (2) landmarks present in the tissue but independent of the cell or structure of interest to make overlay images of LM and EM data. Using this approach, we were able to make accurate 3D-CLEM overlays of liver tissue and correlate the fluorescent signal to the ultrastructural detail provided by the electron microscope. This workflow can be adapted for other dense cellular tissues and thus act as a guide for other three-dimensional correlative studies. LAY DESCRIPTION: As cells and tissues exist in three dimensions, microscopy techniques have been developed to image samples, in 3D, at the highest possible detail. In light microscopy, fluorescent probes are used to identify specific proteins or structures either in live samples, (providing dynamic information), or in fixed slices of tissue. A disadvantage of fluorescence microscopy is that only the labeled proteins/structures are visible, while their cellular context remains hidden. Electron microscopy is able to image biological samples at high resolution and has the advantage that all structures in the tissue are visible at nanometer (10-9 m) resolution. Disadvantages of this technique are that it is more difficult to label a single structure and that the samples must be imaged under high vacuum, so biological samples need to be fixed and embedded in a plastic resin to stay as close to their natural state as possible inside the microscope. Correlative Light and Electron Microscopy aims to combine the advantages of both light and electron microscopy on the same sample. This results in datasets where fluorescent labels can be combined with the high-resolution contextual information provided by the electron microscope. In this study we present a workflow to guide a tissue sample from the light microscope to the electron microscope and image the ultra-structure of a specific cell type in the liver. In particular we focus on the incorporation of fiducial markers during the sample preparation to help navigate through the tissue in 3D in both microscopes. One sample is followed throughout the workflow to visualize the important steps in the process, showing the final result; a dataset combining fluorescent labels with ultra-structural detail.
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Affiliation(s)
- A Kremer
- VIB BioImaging Core, Technologiepark 71, Ghent, 9052, Belgium.,VIB Center for Inflammation Research, Technologiepark 71, Ghent, 9052, Belgium.,Department of Biomedical Molecular Biology, Ghent University, Technologiepark 71, Ghent, 9052, Belgium
| | - E VAN Hamme
- VIB BioImaging Core, Technologiepark 71, Ghent, 9052, Belgium.,VIB Center for Inflammation Research, Technologiepark 71, Ghent, 9052, Belgium.,Department of Biomedical Molecular Biology, Ghent University, Technologiepark 71, Ghent, 9052, Belgium
| | - J Bonnardel
- VIB BioImaging Core, Technologiepark 71, Ghent, 9052, Belgium.,VIB Center for Inflammation Research, Technologiepark 71, Ghent, 9052, Belgium.,Department of Biomedical Molecular Biology, Ghent University, Technologiepark 71, Ghent, 9052, Belgium
| | - P Borghgraef
- VIB BioImaging Core, Technologiepark 71, Ghent, 9052, Belgium.,VIB Center for Inflammation Research, Technologiepark 71, Ghent, 9052, Belgium.,Department of Biomedical Molecular Biology, Ghent University, Technologiepark 71, Ghent, 9052, Belgium
| | - C J GuÉrin
- VIB BioImaging Core, Technologiepark 71, Ghent, 9052, Belgium.,VIB Center for Inflammation Research, Technologiepark 71, Ghent, 9052, Belgium.,Department of Biomedical Molecular Biology, Ghent University, Technologiepark 71, Ghent, 9052, Belgium
| | - M Guilliams
- VIB BioImaging Core, Technologiepark 71, Ghent, 9052, Belgium.,VIB Center for Inflammation Research, Technologiepark 71, Ghent, 9052, Belgium.,Department of Biomedical Molecular Biology, Ghent University, Technologiepark 71, Ghent, 9052, Belgium
| | - S Lippens
- VIB BioImaging Core, Technologiepark 71, Ghent, 9052, Belgium.,VIB Center for Inflammation Research, Technologiepark 71, Ghent, 9052, Belgium.,Department of Biomedical Molecular Biology, Ghent University, Technologiepark 71, Ghent, 9052, Belgium
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17
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Kim E, Lee J, Noh S, Kwon O, Mun JY. Double staining method for array tomography using scanning electron microscopy. Appl Microsc 2020; 50:14. [PMID: 33580409 PMCID: PMC7818292 DOI: 10.1186/s42649-020-00033-8] [Citation(s) in RCA: 0] [Impact Index Per Article: 0] [Reference Citation Analysis] [Abstract] [Key Words] [Track Full Text] [Download PDF] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Received: 04/02/2020] [Accepted: 06/05/2020] [Indexed: 11/16/2022] Open
Abstract
Scanning electron microscopy (SEM) plays a central role in analyzing structures by imaging a large area of brain tissue at nanometer scales. A vast amount of data in the large area are required to study structural changes of cellular organelles in a specific cell, such as neurons, astrocytes, oligodendrocytes, and microglia among brain tissue, at sufficient resolution. Array tomography is a useful method for large-area imaging, and the osmium-thiocarbohydrazide-osmium (OTO) and ferrocyanide-reduced osmium methods are commonly used to enhance membrane contrast. Because many samples prepared using the conventional technique without en bloc staining are considered inadequate for array tomography, we suggested an alternative technique using post-staining conventional samples and compared the advantages.
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Affiliation(s)
- Eunjin Kim
- National Instrumentation Center for Environmental Management, Seoul National University, Seoul, South Korea
| | - Jiyoung Lee
- National Instrumentation Center for Environmental Management, Seoul National University, Seoul, South Korea
| | - Seulgi Noh
- Department of Brain and Cognitive Sciences, Daegu Gyeongbuk Institute of Science & Technology (DGIST), Daegu, South Korea.,Neural circuit research group, Korea Brain Research Institute, Daegu, South Korea
| | - Ohkyung Kwon
- National Instrumentation Center for Environmental Management, Seoul National University, Seoul, South Korea.
| | - Ji Young Mun
- Neural circuit research group, Korea Brain Research Institute, Daegu, South Korea.
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