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Niu Y, Yu Y, Shi X, Fu F, Yang H, Mu Q, Crespy D, Landfester K, Jiang S. In Situ Measurement of Nanoparticle-Blood Protein Adsorption and Its Heterogeneity with Single-Nanoparticle Resolution via Dual Fluorescence Quantification. NANO LETTERS 2024; 24:9202-9211. [PMID: 39037031 DOI: 10.1021/acs.nanolett.4c01469] [Citation(s) in RCA: 0] [Impact Index Per Article: 0] [Reference Citation Analysis] [Abstract] [Key Words] [MESH Headings] [Track Full Text] [Subscribe] [Scholar Register] [Indexed: 07/23/2024]
Abstract
The formation of a protein corona gives nanomedicines a distinct biological identity, profoundly influencing their fate in the body. Nonspecific nanoparticle-protein interactions are typically highly heterogeneous, which can lead to unique biological behaviors and in vivo fates for individual nanoparticles that remain underexplored. To address this, we have established an in situ approach that allows quantitative examination of nanoparticle-protein adsorption at the individual nanoparticle level. This method integrates dual fluorescence quantification techniques, wherein the nanoparticles are first individually analyzed via nanoflow cytometry to detect fluorescent signals from adsorbed proteins. The obtained fluorescence intensity is then translated into protein quantities through calibration with microplate reader quantification. Consequently, this approach enables analysis of interparticle heterogeneity of nano-protein interactions, as well as in situ monitoring of protein adsorption kinetics and nanoparticle aggregation status in blood serum, preconditioning for a comprehensive understanding of nano-bio interactions, and predicting in vivo fate of nanomedicines.
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Affiliation(s)
- Yuanyuan Niu
- Key Laboratory of Marine Drugs, Chinese Ministry of Education, School of Medicine and Pharmacy, Ocean University of China, Qingdao 266003, China
- Laboratory for Marine Drugs and Bioproducts, Qingdao Marine Science and Technology Center, Qingdao 266237, China
| | - Yingjie Yu
- Key Laboratory of Marine Drugs, Chinese Ministry of Education, School of Medicine and Pharmacy, Ocean University of China, Qingdao 266003, China
- Laboratory for Marine Drugs and Bioproducts, Qingdao Marine Science and Technology Center, Qingdao 266237, China
| | - Xinyang Shi
- Key Laboratory of Marine Drugs, Chinese Ministry of Education, School of Medicine and Pharmacy, Ocean University of China, Qingdao 266003, China
- Laboratory for Marine Drugs and Bioproducts, Qingdao Marine Science and Technology Center, Qingdao 266237, China
| | - Fangqin Fu
- Key Laboratory of Marine Drugs, Chinese Ministry of Education, School of Medicine and Pharmacy, Ocean University of China, Qingdao 266003, China
- Laboratory for Marine Drugs and Bioproducts, Qingdao Marine Science and Technology Center, Qingdao 266237, China
| | - Hai Yang
- Department of Pharmacy, Qingdao Central Hospital, University of Health and Rehabilitation Sciences, Qingdao 266042, China
| | - Qiang Mu
- The First Department of Breast Surgery, Qingdao Central Hospital, University of Health and Rehabilitation Sciences (Qingdao Central Medical Group), Qingdao 266042, China
| | - Daniel Crespy
- Department of Materials Science and Engineering, School of Molecular Science and Engineering, Vidyasirimedhi Institute of Science and Technology (VISTEC), Rayong 21210, Thailand
| | - Katharina Landfester
- Max Planck Institute for Polymer Research, Ackermannweg 10, 55128 Mainz, Germany
| | - Shuai Jiang
- Key Laboratory of Marine Drugs, Chinese Ministry of Education, School of Medicine and Pharmacy, Ocean University of China, Qingdao 266003, China
- Laboratory for Marine Drugs and Bioproducts, Qingdao Marine Science and Technology Center, Qingdao 266237, China
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2
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Flormann DAD, Kainka L, Montalvo G, Anton C, Rheinlaender J, Thalla D, Vesperini D, Pohland MO, Kaub KH, Schu M, Pezzano F, Ruprecht V, Terriac E, Hawkins RJ, Lautenschläger F. The structure and mechanics of the cell cortex depend on the location and adhesion state. Proc Natl Acad Sci U S A 2024; 121:e2320372121. [PMID: 39042691 PMCID: PMC11295003 DOI: 10.1073/pnas.2320372121] [Citation(s) in RCA: 0] [Impact Index Per Article: 0] [Reference Citation Analysis] [Abstract] [Key Words] [MESH Headings] [Grants] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Received: 11/28/2023] [Accepted: 06/16/2024] [Indexed: 07/25/2024] Open
Abstract
Cells exist in different phenotypes and can transition between them. A phenotype may be characterized by many different aspects. Here, we focus on the example of whether the cell is adhered or suspended and choose particular parameters related to the structure and mechanics of the actin cortex. The cortex is essential to cell mechanics, morphology, and function, such as for adhesion, migration, and division of animal cells. To predict and control cellular functions and prevent malfunctioning, it is necessary to understand the actin cortex. The structure of the cortex governs cell mechanics; however, the relationship between the architecture and mechanics of the cortex is not yet well enough understood to be able to predict one from the other. Therefore, we quantitatively measured structural and mechanical cortex parameters, including cortical thickness, cortex mesh size, actin bundling, and cortex stiffness. These measurements required developing a combination of measurement techniques in scanning electron, expansion, confocal, and atomic force microscopy. We found that the structure and mechanics of the cortex of cells in interphase are different depending on whether the cell is suspended or adhered. We deduced general correlations between structural and mechanical properties and show how these findings can be explained within the framework of semiflexible polymer network theory. We tested the model predictions by perturbing the properties of the actin within the cortex using compounds. Our work provides an important step toward predictions of cell mechanics from cortical structures and suggests how cortex remodeling between different phenotypes impacts the mechanical properties of cells.
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Affiliation(s)
- D. A. D. Flormann
- Department of Physics, Saarland University, Saarbrücken 66123, Germany
| | - L. Kainka
- Department of Physics, Saarland University, Saarbrücken 66123, Germany
| | - G. Montalvo
- Department of Physics, Saarland University, Saarbrücken 66123, Germany
| | - C. Anton
- Department of Physics, Saarland University, Saarbrücken 66123, Germany
| | - J. Rheinlaender
- Faculty of Science, Institute of Applied Physics, University of Tübingen, Tübingen72076, Germany
| | - D. Thalla
- Department of Physics, Saarland University, Saarbrücken 66123, Germany
| | - D. Vesperini
- Department of Physics, Saarland University, Saarbrücken 66123, Germany
| | - M. O. Pohland
- Department of Physics, Saarland University, Saarbrücken 66123, Germany
| | - K. H. Kaub
- Department of Physics, Saarland University, Saarbrücken 66123, Germany
- Department of Biophysical Chemistry, Georg-August-University, Göttingen37077, Germany
| | - M. Schu
- Department of Physics, Saarland University, Saarbrücken 66123, Germany
| | - F. Pezzano
- Center for Genomic Regulation (CRG), The Barcelona Institute of Science and Technology, Barcelona08003, Spain
| | - V. Ruprecht
- Center for Genomic Regulation (CRG), The Barcelona Institute of Science and Technology, Barcelona08003, Spain
- Universitat Pompeu Fabra, Barcelona08002, Spain
- Institució Catalana de Recerca i Estudis Avançats (ICREA), Barcelona08010, Spain
| | - E. Terriac
- Department of Physics, Saarland University, Saarbrücken 66123, Germany
| | - R. J. Hawkins
- Department of Physics and Astronomy, University of Sheffield, SheffieldS3 7RH, United Kingdom
- African Institute for Mathematical Sciences, Accra20046, Ghana
| | - F. Lautenschläger
- Department of Physics, Saarland University, Saarbrücken 66123, Germany
- Center for Biophysics, Saarland University, Saarbrücken66123, Germany
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3
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Sequeda-Castañeda LG, Suárez-Carvajal LF, Téllez-Corral MA, Gutiérrez-Prieto SJ, Méndez-Pinzón HA. Evaluation of Ilex guayusa and Piper marginatum Extract Cytotoxicity on Human Dental Pulp Mesenchymal Stem Cells. Dent J (Basel) 2024; 12:189. [PMID: 38920890 PMCID: PMC11202831 DOI: 10.3390/dj12060189] [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: 04/29/2024] [Revised: 06/13/2024] [Accepted: 06/18/2024] [Indexed: 06/27/2024] Open
Abstract
BACKGROUND Amelogenesis imperfecta is a hereditary disorder affecting dental enamel. Among its phenotypes, hypocalcified AI is characterized by mineral deficiency, leading to tissue wear and, consequently, dental sensitivity. Excessive fluoride intake (through drinking water, fluoride supplements, toothpaste, or by ingesting products such as pesticides or insecticides) can lead to a condition known as dental fluorosis, which manifests as stains and teeth discoloration affecting their structure. Our recent studies have shown that extracts from Colombian native plants, Ilex guayusa and Piper marginatum, deposit mineral ions such as phosphate and orthophosphate into the dental enamel structure; however, it is unknown whether these extracts produce toxic effects on the dental pulp. OBJECTIVE To assess cytotoxicity effects on human dental pulp stem cells (hDPSCs) exposed to extracts isolated from I. guayusa and P. marginatum and, hence, their safety for clinical use. METHODS Raman spectroscopy, fluorescence microscopy, and flow cytometry techniques were employed. For Raman spectroscopy, hDPSCs were seeded onto nanobiochips designed to provide surface-enhanced Raman spectroscopy (SERS effect), which enhances their Raman signal by several orders of magnitude. After eight days in culture, I. guayusa and P. marginatum extracts at different concentrations (10, 50, and 100 ppm) were added. Raman measurements were performed at 0, 12, and 24 h following extract application. Fluorescence microscopy was conducted using an OLIMPUS fv1000 microscope, a live-dead assay was performed using a kit employing a BD FACS Canto TM II flow cytometer, and data analysis was determined using a FlowJo program. RESULTS The Raman spectroscopy results showed spectra consistent with viable cells. These findings were corroborated using fluorescence microscopy and flow cytometry techniques, confirming high cellular viability. CONCLUSIONS The analyzed extracts exhibited low cytotoxicity, suggesting that they could be safely applied on enamel for remineralization purposes. The use of nanobiochips for SERS effect improved the cell viability assessment.
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Affiliation(s)
- Luis G. Sequeda-Castañeda
- Department of Chemistry, School of Sciences, Pontificia Universidad Javeriana, Bogotá 110231, Colombia;
| | - Luisa F. Suárez-Carvajal
- Oral Rehabilitation, School of Dentistry, Pontificia Universidad Javeriana, Bogotá 110231, Colombia;
| | | | | | - Henry A. Méndez-Pinzón
- Department of Physics, School of Sciences, Pontificia Universidad Javeriana, Bogotá 110231, Colombia
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4
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Coke K, Johnson MJ, Robinson JB, Rettie AJE, Miller TS, Shearing PR. Illuminating Polysulfide Distribution in Lithium Sulfur Batteries; Tracking Polysulfide Shuttle Using Operando Optical Fluorescence Microscopy. ACS APPLIED MATERIALS & INTERFACES 2024; 16. [PMID: 38598420 PMCID: PMC11056927 DOI: 10.1021/acsami.3c14612] [Citation(s) in RCA: 0] [Impact Index Per Article: 0] [Reference Citation Analysis] [Abstract] [Key Words] [Grants] [Track Full Text] [Subscribe] [Scholar Register] [Received: 10/04/2023] [Revised: 03/01/2024] [Accepted: 03/08/2024] [Indexed: 04/12/2024]
Abstract
High-energy-density lithium sulfur (Li-S) batteries suffer heavily from the polysulfide shuttle effect, a result of the dissolution and transport of intermediate polysulfides from the cathode, into the electrolyte, and onto the anode, leading to rapid cell degradation. If this primary mechanism of cell failure is to be overcome, the distribution, dynamics, and degree of polysulfide transport must first be understood in depth. In this work, operando optical fluorescence microscope imaging of optically accessible Li-S cells is shown to enable real-time qualitative visualization of the spatial distribution of lithium polysulfides, both within the electrolyte and porous cathode. Quantitative determinations of spatial concentration are also possible at a low enough concentration. The distribution throughout cycling is monitored, including direct observation of polysulfide shuttling to the anode and consequent dendrite formation. This was enabled through the optimization of a selective fluorescent dye, verified to fluoresce proportionally with concentration of polysulfides within Li-S cells. This ability to directly and conveniently track the spatial distribution of soluble polysulfide intermediates in Li-S battery electrolytes, while the cell operates, has the potential to have a widespread impact across the field, for example, by enabling the influence of a variety of polysulfide mitigation strategies to be assessed and optimized, including in this work the LiNO3 additive.
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Affiliation(s)
- Kofi Coke
- Electrochemical
Innovation Lab, Department of Chemical Engineering, University College London, Torrington Place, London WC1E 7JE, U.K.
| | - Michael J. Johnson
- Electrochemical
Innovation Lab, Department of Chemical Engineering, University College London, Torrington Place, London WC1E 7JE, U.K.
| | - James B. Robinson
- Electrochemical
Innovation Lab, Department of Chemical Engineering, University College London, Torrington Place, London WC1E 7JE, U.K.
- The
Faraday Institution, Quad One, Becquerel Avenue, Harwell Campus, Didcot OX11 ORA, U.K.
- Advanced
Propulsion Lab, UCL East, University College
London, London E15 2JE, U.K.
| | - Alexander J. E. Rettie
- Electrochemical
Innovation Lab, Department of Chemical Engineering, University College London, Torrington Place, London WC1E 7JE, U.K.
- The
Faraday Institution, Quad One, Becquerel Avenue, Harwell Campus, Didcot OX11 ORA, U.K.
- Advanced
Propulsion Lab, UCL East, University College
London, London E15 2JE, U.K.
| | - Thomas S. Miller
- Electrochemical
Innovation Lab, Department of Chemical Engineering, University College London, Torrington Place, London WC1E 7JE, U.K.
- The
Faraday Institution, Quad One, Becquerel Avenue, Harwell Campus, Didcot OX11 ORA, U.K.
| | - Paul R. Shearing
- The
Faraday Institution, Quad One, Becquerel Avenue, Harwell Campus, Didcot OX11 ORA, U.K.
- Department
of Engineering Science, University of Oxford, Parks Road, Oxford OX1 3PJ, U.K.
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Ruiz-Navarro J, Calvo V, Izquierdo M. Extracellular vesicles and microvilli in the immune synapse. Front Immunol 2024; 14:1324557. [PMID: 38268920 PMCID: PMC10806406 DOI: 10.3389/fimmu.2023.1324557] [Citation(s) in RCA: 0] [Impact Index Per Article: 0] [Reference Citation Analysis] [Abstract] [Key Words] [MESH Headings] [Grants] [Track Full Text] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Received: 10/19/2023] [Accepted: 12/05/2023] [Indexed: 01/26/2024] Open
Abstract
T cell receptor (TCR) binding to cognate antigen on the plasma membrane of an antigen-presenting cell (APC) triggers the immune synapse (IS) formation. The IS constitutes a dedicated contact region between different cells that comprises a signaling platform where several cues evoked by TCR and accessory molecules are integrated, ultimately leading to an effective TCR signal transmission that guarantees intercellular message communication. This eventually leads to T lymphocyte activation and the efficient execution of different T lymphocyte effector tasks, including cytotoxicity and subsequent target cell death. Recent evidence demonstrates that the transmission of information between immune cells forming synapses is produced, to a significant extent, by the generation and secretion of distinct extracellular vesicles (EV) from both the effector T lymphocyte and the APC. These EV carry biologically active molecules that transfer cues among immune cells leading to a broad range of biological responses in the recipient cells. Included among these bioactive molecules are regulatory miRNAs, pro-apoptotic molecules implicated in target cell apoptosis, or molecules triggering cell activation. In this study we deal with the different EV classes detected at the IS, placing emphasis on the most recent findings on microvilli/lamellipodium-produced EV. The signals leading to polarized secretion of EV at the synaptic cleft will be discussed, showing that the IS architecture fulfills a fundamental task during this route.
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Affiliation(s)
- Javier Ruiz-Navarro
- Department of Metabolism and Cell Signaling, Instituto de Investigaciones Biomédicas Sols-Morreale (IIBM), Consejo Superior de Investigaciones Científicas (CSIC)-Universidad Autónoma de Madrid (UAM), Madrid, Spain
| | - Víctor Calvo
- Departamento de Bioquímica, Facultad de Medicina, Universidad Autónoma de Madrid (UAM), Madrid, Spain
| | - Manuel Izquierdo
- Department of Metabolism and Cell Signaling, Instituto de Investigaciones Biomédicas Sols-Morreale (IIBM), Consejo Superior de Investigaciones Científicas (CSIC)-Universidad Autónoma de Madrid (UAM), Madrid, Spain
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6
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Jose A, Cheung PY, Laouby Z, Vanholsbeeck F, Cheyne JE. Low-cost reversible tandem lens mesoscope for brain imaging in rodents. NEUROPHOTONICS 2024; 11:014306. [PMID: 38464865 PMCID: PMC10924044 DOI: 10.1117/1.nph.11.1.014306] [Citation(s) in RCA: 0] [Impact Index Per Article: 0] [Reference Citation Analysis] [Abstract] [Key Words] [Track Full Text] [Figures] [Subscribe] [Scholar Register] [Received: 04/25/2023] [Revised: 02/07/2024] [Accepted: 02/09/2024] [Indexed: 03/12/2024]
Abstract
Significance The development of imaging systems that are cost-efficient and modular is essential for modern neuroscience research. Aim In the current study, we designed, developed, and characterized a low-cost reversible tandem lens mesoscope for brain imaging in rodents. Approach Using readily available components, we assembled a robust imaging system that is highly efficient and cost-effective. We developed a mesoscope that offers high-resolution structural and functional imaging with cost-effective lenses and CMOS camera. Results The reversible tandem lens configuration of the mesoscope offers two fields of view (FOVs), which can be achieved by swapping the objective and imaging lenses. The large FOV configuration of 12.6 × 10.5 mm provides a spatial resolution up to 4.92 μ m , and the small FOV configuration of 6 × 5 mm provides a resolution of up to 2.46 μ m . We demonstrate the efficiency of our system for imaging neuronal calcium activity in both rat and mouse brains in vivo. Conclusions The careful selection of the mesoscope components ensured its compactness, portability, and versatility, meaning that different types of samples and sample holders can be easily accommodated, enabling a range of different experiments both in vivo and in vitro. The custom-built reversible FOV mesoscope is cost-effective and was developed for under US$10,000 with excellent performance.
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Affiliation(s)
- Ashly Jose
- University of Auckland, Department of Physics, Auckland, New Zealand
- Dodd-Walls Centre for Photonic and Quantum Technologies (DWC), Dunedin, New Zealand
| | - Pang Ying Cheung
- Dodd-Walls Centre for Photonic and Quantum Technologies (DWC), Dunedin, New Zealand
- University of Auckland, Department of Physiology, Auckland, New Zealand
| | - Zahra Laouby
- Dodd-Walls Centre for Photonic and Quantum Technologies (DWC), Dunedin, New Zealand
- University of Auckland, Department of Physiology, Auckland, New Zealand
| | - Frédérique Vanholsbeeck
- University of Auckland, Department of Physics, Auckland, New Zealand
- Dodd-Walls Centre for Photonic and Quantum Technologies (DWC), Dunedin, New Zealand
| | - Juliette E. Cheyne
- Dodd-Walls Centre for Photonic and Quantum Technologies (DWC), Dunedin, New Zealand
- University of Auckland, Department of Physiology, Auckland, New Zealand
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7
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Gu Y, Koch J, Garnier C, Erny A, Lozach PY. Making Rift Valley Fever Viral Particles Fluorescent. Methods Mol Biol 2024; 2824:165-188. [PMID: 39039413 DOI: 10.1007/978-1-0716-3926-9_12] [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: 07/24/2024]
Abstract
Rift Valley fever virus (RVFV) is a mosquito-borne pathogen that represents a significant threat to both human and veterinary public health. Since its discovery in the Great Rift Valley of Kenya in the 1930s, the virus has spread across Africa and beyond, now posing a risk of introduction into Southern Europe and Asia. Despite recent progresses, early RVFV-host cell interactions remain largely uncharacterized. In this method chapter, we delineate the procedure for labeling RVFV particles with fluorescent organic dyes. This approach makes it feasible to visualize single viral particles in both fixed and living cells and study RVFV entry into host cells. We provide additional examples with two viruses closely related to RVFV, namely, Toscana virus and Uukuniemi virus. Furthermore, we illustrate how to utilize fluorescent viral particles to examine and quantify each step of the cell entry program of RVFV, which includes state-of-the-art fluorescence-based detection techniques such as fluorescence microscopy, flow cytometry, and fluorimetry.
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Affiliation(s)
- Yu Gu
- IVPC UMR754, INRAE, Université Claude Bernard Lyon 1, EPHE, PSL Research University, Lyon, France
| | - Jana Koch
- IVPC UMR754, INRAE, Université Claude Bernard Lyon 1, EPHE, PSL Research University, Lyon, France
| | - Céline Garnier
- IVPC UMR754, INRAE, Université Claude Bernard Lyon 1, EPHE, PSL Research University, Lyon, France
| | - Alexandra Erny
- IVPC UMR754, INRAE, Université Claude Bernard Lyon 1, EPHE, PSL Research University, Lyon, France
| | - Pierre-Yves Lozach
- IVPC UMR754, INRAE, Université Claude Bernard Lyon 1, EPHE, PSL Research University, Lyon, France.
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8
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Brownsey DK, Gafuik CJ, Kim DS, O'Sullivan L, Gorobets E, Krukowski S, Turk M, Jenne CN, Mahoney DJ, Derksen DJ. Utilising the intrinsic fluorescence of pomalidomide for imaging applications. Chem Commun (Camb) 2023; 59:14532-14535. [PMID: 38019727 DOI: 10.1039/d3cc04314b] [Citation(s) in RCA: 0] [Impact Index Per Article: 0] [Reference Citation Analysis] [Abstract] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Indexed: 12/01/2023]
Abstract
Optimisation of protein degraders requires balancing multiple factors including potency, cell permeability and solubility. Here we show that the fluorescence of pomalidomide can be used in high-throughput screening assays to rapidly assess cellular penetration of degrader candidates. In addition, this technique can be paired with endocytosis inhibitors to gain insight into potential mechanisms of candidates entering a target cell. A model library of pomalidomide conjugates was synthesised and evaluated using high-throughput fluorescence microscopy. This technique based on intrinsic fluorescence can be used to guide rational design of pomalidomide conjugates without the need for additional labels or tags.
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Affiliation(s)
- Duncan K Brownsey
- Department of Chemistry, University of Calgary, Calgary, AB, Canada
- Alberta Children's Health Research Institute (ACHRI), University of Calgary, Calgary, AB, Canada
- Arnie Charbonneau Cancer Institute, University of Calgary, Calgary, AB, Canada
| | - Christopher J Gafuik
- Alberta Children's Health Research Institute (ACHRI), University of Calgary, Calgary, AB, Canada
- Arnie Charbonneau Cancer Institute, University of Calgary, Calgary, AB, Canada
- Department of Biochemistry and Molecular Biology, University of Calgary, Calgary, AB, Canada
- Microbiology, Immunology and Infectious Diseases, University of Calgary, Calgary, Alberta, Canada
| | - Dae-Sun Kim
- Alberta Children's Health Research Institute (ACHRI), University of Calgary, Calgary, AB, Canada
- Arnie Charbonneau Cancer Institute, University of Calgary, Calgary, AB, Canada
- Department of Biochemistry and Molecular Biology, University of Calgary, Calgary, AB, Canada
- Microbiology, Immunology and Infectious Diseases, University of Calgary, Calgary, Alberta, Canada
| | - Leonie O'Sullivan
- Department of Chemistry, University of Calgary, Calgary, AB, Canada
- Alberta Children's Health Research Institute (ACHRI), University of Calgary, Calgary, AB, Canada
- Arnie Charbonneau Cancer Institute, University of Calgary, Calgary, AB, Canada
| | - Evgueni Gorobets
- Department of Chemistry, University of Calgary, Calgary, AB, Canada
- Alberta Children's Health Research Institute (ACHRI), University of Calgary, Calgary, AB, Canada
- Arnie Charbonneau Cancer Institute, University of Calgary, Calgary, AB, Canada
| | - Samuel Krukowski
- Department of Chemistry, University of Calgary, Calgary, AB, Canada
- Alberta Children's Health Research Institute (ACHRI), University of Calgary, Calgary, AB, Canada
- Arnie Charbonneau Cancer Institute, University of Calgary, Calgary, AB, Canada
| | - Madison Turk
- Microbiology, Immunology and Infectious Diseases, University of Calgary, Calgary, Alberta, Canada
- Calvin, Phoebe, and Joan Snyder Institute for Chronic Diseases, University of Calgary, Calgary, AB, Canada
| | - Craig N Jenne
- Microbiology, Immunology and Infectious Diseases, University of Calgary, Calgary, Alberta, Canada
- Calvin, Phoebe, and Joan Snyder Institute for Chronic Diseases, University of Calgary, Calgary, AB, Canada
| | - Douglas J Mahoney
- Alberta Children's Health Research Institute (ACHRI), University of Calgary, Calgary, AB, Canada
- Arnie Charbonneau Cancer Institute, University of Calgary, Calgary, AB, Canada
- Department of Biochemistry and Molecular Biology, University of Calgary, Calgary, AB, Canada
- Microbiology, Immunology and Infectious Diseases, University of Calgary, Calgary, Alberta, Canada
| | - Darren J Derksen
- Department of Chemistry, University of Calgary, Calgary, AB, Canada
- Alberta Children's Health Research Institute (ACHRI), University of Calgary, Calgary, AB, Canada
- Arnie Charbonneau Cancer Institute, University of Calgary, Calgary, AB, Canada
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Yang E, Shen XE, West‐Foyle H, Hahm T, Siegler MA, Brown DR, Johnson CC, Kim JH, Roker LA, Tressler CM, Barman I, Kuo SC, Glunde K. FluoMALDI Microscopy: Matrix Co-Crystallization Simultaneously Enhances Fluorescence and MALDI Imaging. ADVANCED SCIENCE (WEINHEIM, BADEN-WURTTEMBERG, GERMANY) 2023; 10:e2304343. [PMID: 37908150 PMCID: PMC10724403 DOI: 10.1002/advs.202304343] [Citation(s) in RCA: 0] [Impact Index Per Article: 0] [Reference Citation Analysis] [Abstract] [Key Words] [MESH Headings] [Grants] [Track Full Text] [Subscribe] [Scholar Register] [Received: 06/28/2023] [Revised: 09/15/2023] [Indexed: 11/02/2023]
Abstract
Here, the authors report that co-crystallization of fluorophores with matrix-assisted laser desorption/ionization (MALDI) imaging matrices significantly enhances fluorophore brightness up to 79-fold, enabling the amplification of innate tissue autofluorescence. This discovery facilitates FluoMALDI, the imaging of the same biological sample by both fluorescence microscopy and MALDI imaging. The approach combines the high spatial resolution and specific labeling capabilities of fluorescence microscopy with the inherently multiplexed, versatile imaging capabilities of MALDI imaging. This new paradigm simplifies registration by avoiding physical changes between fluorescence and MALDI imaging, allowing to image the exact same cells in tissues with both modalities. Matrix-fluorophore co-crystallization also facilitates applications with insufficient fluorescence brightness. The authors demonstrate feasibility of FluoMALDI imaging with endogenous and exogenous fluorophores and autofluorescence-based FluoMALDI of brain and kidney tissue sections. FluoMALDI will advance structural-functional microscopic imaging in cell biology, biomedicine, and pathology.
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Affiliation(s)
- Ethan Yang
- Russell H. Morgan Department of Radiology and Radiological ScienceJohns Hopkins University School of MedicineBaltimoreMD21287USA
- Applied Imaging Mass Spectrometry CoreJohns Hopkins University School of MedicineBaltimoreMD21287USA
| | - Xinyi Elaine Shen
- Russell H. Morgan Department of Radiology and Radiological ScienceJohns Hopkins University School of MedicineBaltimoreMD21287USA
- Applied Imaging Mass Spectrometry CoreJohns Hopkins University School of MedicineBaltimoreMD21287USA
| | - Hoku West‐Foyle
- Microscope FacilityJohns Hopkins University School of MedicineBaltimoreMD21205USA
- Department of Cell BiologyJohns Hopkins University School of MedicineBaltimoreMD21205USA
| | - Tae‐Hun Hahm
- Russell H. Morgan Department of Radiology and Radiological ScienceJohns Hopkins University School of MedicineBaltimoreMD21287USA
- Applied Imaging Mass Spectrometry CoreJohns Hopkins University School of MedicineBaltimoreMD21287USA
| | | | - Dalton R. Brown
- Russell H. Morgan Department of Radiology and Radiological ScienceJohns Hopkins University School of MedicineBaltimoreMD21287USA
- Applied Imaging Mass Spectrometry CoreJohns Hopkins University School of MedicineBaltimoreMD21287USA
| | - Cole C. Johnson
- Russell H. Morgan Department of Radiology and Radiological ScienceJohns Hopkins University School of MedicineBaltimoreMD21287USA
- Applied Imaging Mass Spectrometry CoreJohns Hopkins University School of MedicineBaltimoreMD21287USA
| | - Jeong Hee Kim
- Department of Mechanical EngineeringJohns Hopkins UniversityBaltimoreMD21218USA
| | - LaToya Ann Roker
- Microscope FacilityJohns Hopkins University School of MedicineBaltimoreMD21205USA
- Department of Cell BiologyJohns Hopkins University School of MedicineBaltimoreMD21205USA
| | - Caitlin M. Tressler
- Russell H. Morgan Department of Radiology and Radiological ScienceJohns Hopkins University School of MedicineBaltimoreMD21287USA
- Applied Imaging Mass Spectrometry CoreJohns Hopkins University School of MedicineBaltimoreMD21287USA
| | - Ishan Barman
- Russell H. Morgan Department of Radiology and Radiological ScienceJohns Hopkins University School of MedicineBaltimoreMD21287USA
- Department of Mechanical EngineeringJohns Hopkins UniversityBaltimoreMD21218USA
- Sidney Kimmel Comprehensive Cancer CancerJohns Hopkins University School of MedicineBaltimoreMD21231USA
| | - Scot C. Kuo
- Microscope FacilityJohns Hopkins University School of MedicineBaltimoreMD21205USA
- Department of Cell BiologyJohns Hopkins University School of MedicineBaltimoreMD21205USA
- Department of Biomedical EngineeringJohns Hopkins University School of MedicineBaltimoreMD21218USA
| | - Kristine Glunde
- Russell H. Morgan Department of Radiology and Radiological ScienceJohns Hopkins University School of MedicineBaltimoreMD21287USA
- Applied Imaging Mass Spectrometry CoreJohns Hopkins University School of MedicineBaltimoreMD21287USA
- Sidney Kimmel Comprehensive Cancer CancerJohns Hopkins University School of MedicineBaltimoreMD21231USA
- Department of Biological ChemistryJohns Hopkins University School of MedicineBaltimoreMD21205USA
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10
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Graziotto ME, Kidman CJ, Adair LD, James SA, Harris HH, New EJ. Towards multimodal cellular imaging: optical and X-ray fluorescence. Chem Soc Rev 2023; 52:8295-8318. [PMID: 37910139 DOI: 10.1039/d3cs00509g] [Citation(s) in RCA: 3] [Impact Index Per Article: 3.0] [Reference Citation Analysis] [Abstract] [MESH Headings] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Indexed: 11/03/2023]
Abstract
Imaging techniques permit the study of the molecular interactions that underlie health and disease. Each imaging technique collects unique chemical information about the cellular environment. Multimodal imaging, using a single probe that can be detected by multiple imaging modalities, can maximise the information extracted from a single cellular sample by combining the results of different imaging techniques. Of particular interest in biological imaging is the combination of the specificity and sensitivity of optical fluorescence microscopy (OFM) with the quantitative and element-specific nature of X-ray fluorescence microscopy (XFM). Together, these techniques give a greater understanding of how native elements or therapeutics affect the cellular environment. This review focuses on recent studies where both techniques were used in conjunction to study cellular systems, demonstrating the breadth of biological models to which this combination of techniques can be applied and the potential for these techniques to unlock untapped knowledge of disease states.
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Affiliation(s)
- Marcus E Graziotto
- School of Chemistry, The University of Sydney, Sydney, NSW, 2006, Australia.
| | - Clinton J Kidman
- Department of Chemistry, The University of Adelaide, Adelaide, SA, 5005, Australia
| | - Liam D Adair
- School of Chemistry, The University of Sydney, Sydney, NSW, 2006, Australia.
- Sydney Nano Institute, The University of Sydney, Sydney, NSW, 2006, Australia
- Australian Research Council Centre of Excellence for Innovations in Peptide and Protein Science, The University of Sydney, Sydney, NSW, 2006, Australia
| | - Simon A James
- Australian Nuclear Science and Technology Organisation, Clayton, Victoria, 3168, Australia
| | - Hugh H Harris
- Department of Chemistry, The University of Adelaide, Adelaide, SA, 5005, Australia
| | - Elizabeth J New
- School of Chemistry, The University of Sydney, Sydney, NSW, 2006, Australia.
- Sydney Nano Institute, The University of Sydney, Sydney, NSW, 2006, Australia
- Australian Research Council Centre of Excellence for Innovations in Peptide and Protein Science, The University of Sydney, Sydney, NSW, 2006, Australia
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11
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Tadesse K, Mandracchia B, Yoon K, Han K, Jia S. Three-dimensional multifocal scanning microscopy for super-resolution cell and tissue imaging. OPTICS EXPRESS 2023; 31:38550-38559. [PMID: 38017958 DOI: 10.1364/oe.501100] [Citation(s) in RCA: 0] [Impact Index Per Article: 0] [Reference Citation Analysis] [Abstract] [MESH Headings] [Grants] [Track Full Text] [Subscribe] [Scholar Register] [Received: 07/19/2023] [Accepted: 10/24/2023] [Indexed: 11/30/2023]
Abstract
Recent advancements in image-scanning microscopy have significantly enriched super-resolution biological research, providing deeper insights into cellular structures and processes. However, current image-scanning techniques often require complex instrumentation and alignment, constraining their broader applicability in cell biological discovery and convenient, cost-effective integration into commonly used frameworks like epi-fluorescence microscopes. Here, we introduce three-dimensional multifocal scanning microscopy (3D-MSM) for super-resolution imaging of cells and tissue with substantially reduced instrumental complexity. This method harnesses the inherent 3D movement of specimens to achieve stationary, multi-focal excitation and super-resolution microscopy through a standard epi-fluorescence platform. We validated the system using a range of phantom, single-cell, and tissue specimens. The combined strengths of structured illumination, confocal detection, and epi-fluorescence setup result in two-fold resolution improvement in all three dimensions, effective optical sectioning, scalable volume acquisition, and compatibility with general imaging and sample protocols. We anticipate that 3D-MSM will pave a promising path for future super-resolution investigations in cell and tissue biology.
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12
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Li Z, Hasson A, Daggumati L, Zhang H, Thorek DLJ. Molecular Imaging of ACE2 Expression in Infectious Disease and Cancer. Viruses 2023; 15:1982. [PMID: 37896761 PMCID: PMC10610869 DOI: 10.3390/v15101982] [Citation(s) in RCA: 0] [Impact Index Per Article: 0] [Reference Citation Analysis] [Abstract] [Key Words] [MESH Headings] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Received: 08/23/2023] [Revised: 09/18/2023] [Accepted: 09/20/2023] [Indexed: 10/29/2023] Open
Abstract
Angiotensin-converting enzyme 2 (ACE2) is a cell-surface receptor that plays a critical role in the pathogenesis of SARS-CoV-2 infection. Through the use of ligands engineered for the receptor, ACE2 imaging has emerged as a valuable tool for preclinical and clinical research. These can be used to visualize the expression and distribution of ACE2 in tissues and cells. A variety of techniques including optical, magnetic resonance, and nuclear medicine contrast agents have been developed and employed in the preclinical setting. Positron-emitting radiotracers for highly sensitive and quantitative tomography have also been translated in the context of SARS-CoV-2-infected and control patients. Together this information can be used to better understand the mechanisms of SARS-CoV-2 infection, the potential roles of ACE2 in homeostasis and disease, and to identify potential therapeutic modulators in infectious disease and cancer. This review summarizes the tools and techniques to detect and delineate ACE2 in this rapidly expanding field.
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Affiliation(s)
- Zhiyao Li
- Mallinckrodt Institute of Radiology, Washington University in St. Louis School of Medicine, St. Louis, MO 63110, USA; (Z.L.); (A.H.); (H.Z.)
- Program in Quantitative Molecular Therapeutics, Washington University in St. Louis School of Medicine, St. Louis, MO 63110, USA;
| | - Abbie Hasson
- Mallinckrodt Institute of Radiology, Washington University in St. Louis School of Medicine, St. Louis, MO 63110, USA; (Z.L.); (A.H.); (H.Z.)
- Program in Quantitative Molecular Therapeutics, Washington University in St. Louis School of Medicine, St. Louis, MO 63110, USA;
- Department of Biomedical Engineering, Washington University, St. Louis, MO 63110, USA
| | - Lasya Daggumati
- Program in Quantitative Molecular Therapeutics, Washington University in St. Louis School of Medicine, St. Louis, MO 63110, USA;
- School of Medicine Missouri, University of Missouri-Kansas City, Kansas, MO 64108, USA
| | - Hanwen Zhang
- Mallinckrodt Institute of Radiology, Washington University in St. Louis School of Medicine, St. Louis, MO 63110, USA; (Z.L.); (A.H.); (H.Z.)
- Program in Quantitative Molecular Therapeutics, Washington University in St. Louis School of Medicine, St. Louis, MO 63110, USA;
- Siteman Cancer Center, St. Louis, MO 63110, USA
| | - Daniel L. J. Thorek
- Mallinckrodt Institute of Radiology, Washington University in St. Louis School of Medicine, St. Louis, MO 63110, USA; (Z.L.); (A.H.); (H.Z.)
- Program in Quantitative Molecular Therapeutics, Washington University in St. Louis School of Medicine, St. Louis, MO 63110, USA;
- Department of Biomedical Engineering, Washington University, St. Louis, MO 63110, USA
- Siteman Cancer Center, St. Louis, MO 63110, USA
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13
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Peters JP, Brahms A, Janicaud V, Anikeeva M, Peschke E, Ellermann F, Ferrari A, Hellmold D, Held-Feindt J, Kim NM, Meiser J, Aden K, Herges R, Hövener JB, Pravdivtsev AN. Nitrogen-15 dynamic nuclear polarization of nicotinamide derivatives in biocompatible solutions. SCIENCE ADVANCES 2023; 9:eadd3643. [PMID: 37611105 PMCID: PMC10446501 DOI: 10.1126/sciadv.add3643] [Citation(s) in RCA: 0] [Impact Index Per Article: 0] [Reference Citation Analysis] [Abstract] [MESH Headings] [Grants] [Track Full Text] [Subscribe] [Scholar Register] [Received: 05/17/2023] [Accepted: 07/21/2023] [Indexed: 08/25/2023]
Abstract
Dissolution dynamic nuclear polarization (dDNP) increases the sensitivity of magnetic resonance imaging by more than 10,000 times, enabling in vivo metabolic imaging to be performed noninvasively in real time. Here, we are developing a group of dDNP polarized tracers based on nicotinamide (NAM). We synthesized 1-15N-NAM and 1-15N nicotinic acid and hyperpolarized them with dDNP, reaching (13.0 ± 1.9)% 15N polarization. We found that the lifetime of hyperpolarized 1-15N-NAM is strongly field- and pH-dependent, with T1 being as long as 41 s at a pH of 12 and 1 T while as short as a few seconds at neutral pH and fields below 1 T. The remarkably short 1-15N lifetime at low magnetic fields and neutral pH drove us to establish a unique pH neutralization procedure. Using 15N dDNP and an inexpensive rodent imaging probe designed in-house, we acquired a 15N MRI of 1-15N-NAM (previously hyperpolarized for more than an hour) in less than 1 s.
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Affiliation(s)
- Josh P. Peters
- Section Biomedical Imaging, Molecular Imaging North Competence Center (MOIN CC), Department of Radiology and Neuroradiology, University Medical Center Kiel, Kiel University, Am Botanischen Garten 14, 24118 Kiel, Germany
| | - Arne Brahms
- Otto Diels Institute for Organic Chemistry, Kiel University, Otto-Hahn Platz 4, 24098 Kiel, Germany
| | - Vivian Janicaud
- Section Biomedical Imaging, Molecular Imaging North Competence Center (MOIN CC), Department of Radiology and Neuroradiology, University Medical Center Kiel, Kiel University, Am Botanischen Garten 14, 24118 Kiel, Germany
| | - Maria Anikeeva
- Section Biomedical Imaging, Molecular Imaging North Competence Center (MOIN CC), Department of Radiology and Neuroradiology, University Medical Center Kiel, Kiel University, Am Botanischen Garten 14, 24118 Kiel, Germany
| | - Eva Peschke
- Section Biomedical Imaging, Molecular Imaging North Competence Center (MOIN CC), Department of Radiology and Neuroradiology, University Medical Center Kiel, Kiel University, Am Botanischen Garten 14, 24118 Kiel, Germany
| | - Frowin Ellermann
- Section Biomedical Imaging, Molecular Imaging North Competence Center (MOIN CC), Department of Radiology and Neuroradiology, University Medical Center Kiel, Kiel University, Am Botanischen Garten 14, 24118 Kiel, Germany
| | - Arianna Ferrari
- Section Biomedical Imaging, Molecular Imaging North Competence Center (MOIN CC), Department of Radiology and Neuroradiology, University Medical Center Kiel, Kiel University, Am Botanischen Garten 14, 24118 Kiel, Germany
| | - Dana Hellmold
- Department of Neurosurgery, University Medical Center Kiel, Arnold-Heller-Str. 3, House D, 24105 Kiel, Germany
| | - Janka Held-Feindt
- Department of Neurosurgery, University Medical Center Kiel, Arnold-Heller-Str. 3, House D, 24105 Kiel, Germany
| | - Na-mi Kim
- Institute of Clinical Molecular Biology, Kiel University, Rosalind-Franklin-Straße 12, 24105 Kiel, Germany
| | - Johannes Meiser
- Cancer Metabolism Group, Department of Cancer Research, Luxembourg Institute of Health, 6A Rue Nicolas-Ernest Barblé, 1210 Luxembourg, Luxembourg
| | - Konrad Aden
- Institute of Clinical Molecular Biology, Kiel University, Rosalind-Franklin-Straße 12, 24105 Kiel, Germany
- Department of Internal Medicine I, University Medical Center Kiel, Kiel, Germany
| | - Rainer Herges
- Otto Diels Institute for Organic Chemistry, Kiel University, Otto-Hahn Platz 4, 24098 Kiel, Germany
| | - Jan-Bernd Hövener
- Section Biomedical Imaging, Molecular Imaging North Competence Center (MOIN CC), Department of Radiology and Neuroradiology, University Medical Center Kiel, Kiel University, Am Botanischen Garten 14, 24118 Kiel, Germany
| | - Andrey N. Pravdivtsev
- Section Biomedical Imaging, Molecular Imaging North Competence Center (MOIN CC), Department of Radiology and Neuroradiology, University Medical Center Kiel, Kiel University, Am Botanischen Garten 14, 24118 Kiel, Germany
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14
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Sanders S, Jensen Y, Reimer R, Bosse JB. From the beginnings to multidimensional light and electron microscopy of virus morphogenesis. Adv Virus Res 2023; 116:45-88. [PMID: 37524482 DOI: 10.1016/bs.aivir.2023.05.001] [Citation(s) in RCA: 0] [Impact Index Per Article: 0] [Reference Citation Analysis] [Abstract] [Key Words] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Indexed: 08/02/2023]
Abstract
Individual functional viral morphogenesis events are often dynamic, short, and infrequent and might be obscured by other pathways and dead-end products. Volumetric live cell imaging has become an essential tool for studying viral morphogenesis events. It allows following entire dynamic processes while providing functional evidence that the imaged process is involved in viral production. Moreover, it allows to capture many individual events and allows quantitative analysis. Finally, the correlation of volumetric live-cell data with volumetric electron microscopy (EM) can provide crucial insights into the ultrastructure and mechanisms of viral morphogenesis events. Here, we provide an overview and discussion of suitable imaging methods for volumetric correlative imaging of viral morphogenesis and frame them in a historical summary of their development.
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Affiliation(s)
- Saskia Sanders
- Department of Virology, Hannover Medical School, Hannover, Germany; Leibniz Institute of Virology (LIV), Hamburg, Germany; Centre for Structural Systems Biology, Hamburg, Germany; Cluster of Excellence RESIST (EXC 2155), Hannover Medical School, Hannover, Germany
| | - Yannick Jensen
- Department of Virology, Hannover Medical School, Hannover, Germany; Leibniz Institute of Virology (LIV), Hamburg, Germany; Centre for Structural Systems Biology, Hamburg, Germany; Cluster of Excellence RESIST (EXC 2155), Hannover Medical School, Hannover, Germany
| | | | - Jens B Bosse
- Department of Virology, Hannover Medical School, Hannover, Germany; Leibniz Institute of Virology (LIV), Hamburg, Germany; Centre for Structural Systems Biology, Hamburg, Germany; Cluster of Excellence RESIST (EXC 2155), Hannover Medical School, Hannover, Germany.
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15
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Fernández-Galiana Á, Bibikova O, Vilms Pedersen S, Stevens MM. Fundamentals and Applications of Raman-Based Techniques for the Design and Development of Active Biomedical Materials. ADVANCED MATERIALS (DEERFIELD BEACH, FLA.) 2023:e2210807. [PMID: 37001970 DOI: 10.1002/adma.202210807] [Citation(s) in RCA: 0] [Impact Index Per Article: 0] [Reference Citation Analysis] [Abstract] [Key Words] [Grants] [Track Full Text] [Subscribe] [Scholar Register] [Received: 11/21/2022] [Revised: 03/03/2023] [Indexed: 06/19/2023]
Abstract
Raman spectroscopy is an analytical method based on light-matter interactions that can interrogate the vibrational modes of matter and provide representative molecular fingerprints. Mediated by its label-free, non-invasive nature, and high molecular specificity, Raman-based techniques have become ubiquitous tools for in situ characterization of materials. This review comprehensively describes the theoretical and practical background of Raman spectroscopy and its advanced variants. The numerous facets of material characterization that Raman scattering can reveal, including biomolecular identification, solid-to-solid phase transitions, and spatial mapping of biomolecular species in bioactive materials, are highlighted. The review illustrates the potential of these techniques in the context of active biomedical material design and development by highlighting representative studies from the literature. These studies cover the use of Raman spectroscopy for the characterization of both natural and synthetic biomaterials, including engineered tissue constructs, biopolymer systems, ceramics, and nanoparticle formulations, among others. To increase the accessibility and adoption of these techniques, the present review also provides the reader with practical recommendations on the integration of Raman techniques into the experimental laboratory toolbox. Finally, perspectives on how recent developments in plasmon- and coherently-enhanced Raman spectroscopy can propel Raman from underutilized to critical for biomaterial development are provided.
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Affiliation(s)
- Álvaro Fernández-Galiana
- Department of Materials, Department of Bioengineering, Imperial College London, SW7 2AZ, London, UK
| | - Olga Bibikova
- Department of Materials, Department of Bioengineering, Imperial College London, SW7 2AZ, London, UK
| | - Simon Vilms Pedersen
- Department of Materials, Department of Bioengineering, Imperial College London, SW7 2AZ, London, UK
| | - Molly M Stevens
- Department of Materials, Department of Bioengineering, Imperial College London, SW7 2AZ, London, UK
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16
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Jadhav AC, Kounatidis I. Correlative Cryo-imaging Using Soft X-Ray Tomography for the Study of Virus Biology in Cells and Tissues. Subcell Biochem 2023; 106:169-196. [PMID: 38159227 DOI: 10.1007/978-3-031-40086-5_6] [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: 01/03/2024]
Abstract
Viruses are obligate intracellular pathogens that depend on their host cell machinery and metabolism for their replicative life cycle. Virus entry, replication, and assembly are dynamic processes that lead to the reorganisation of host cell components. Therefore, a complete understanding of the viral processes requires their study in the cellular context where advanced imaging has been proven valuable in providing the necessary information. Among the available imaging techniques, soft X-ray tomography (SXT) at cryogenic temperatures can provide three-dimensional mapping to 25 nm resolution and is ideally suited to visualise the internal organisation of virus-infected cells. In this chapter, the principles and practices of synchrotron-based cryo-soft X-ray tomography (cryo-SXT) in virus research are presented. The potential of the cryo-SXT in correlative microscopy platforms is also demonstrated through working examples of reovirus and hepatitis research at Beamline B24 (Diamond Light Source Synchrotron, UK) and BL09-Mistral beamline (ALBA Synchrotron, Spain), respectively.
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Affiliation(s)
- Archana C Jadhav
- Beamline B24, Diamond Light Source, Harwell Science and Innovation Campus, Didcot, UK
| | - Ilias Kounatidis
- Beamline B24, Diamond Light Source, Harwell Science and Innovation Campus, Didcot, UK.
- School of Life, Health and Chemical Sciences, The Open University, Milton Keynes, UK.
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17
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Santos R, Ástvaldsson Á, Pipaliya SV, Zumthor JP, Dacks JB, Svärd S, Hehl AB, Faso C. Combined nanometric and phylogenetic analysis of unique endocytic compartments in Giardia lamblia sheds light on the evolution of endocytosis in Metamonada. BMC Biol 2022; 20:206. [PMID: 36127707 PMCID: PMC9490929 DOI: 10.1186/s12915-022-01402-3] [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: 05/06/2022] [Accepted: 09/06/2022] [Indexed: 11/27/2022] Open
Abstract
Background Giardia lamblia, a parasitic protist of the Metamonada supergroup, has evolved one of the most diverged endocytic compartment systems investigated so far. Peripheral endocytic compartments, currently known as peripheral vesicles or vacuoles (PVs), perform bulk uptake of fluid phase material which is then digested and sorted either to the cell cytosol or back to the extracellular space. Results Here, we present a quantitative morphological characterization of these organelles using volumetric electron microscopy and super-resolution microscopy (SRM). We defined a morphological classification for the heterogenous population of PVs and performed a comparative analysis of PVs and endosome-like organelles in representatives of phylogenetically related taxa, Spironucleus spp. and Tritrichomonas foetus. To investigate the as-yet insufficiently understood connection between PVs and clathrin assemblies in G. lamblia, we further performed an in-depth search for two key elements of the endocytic machinery, clathrin heavy chain (CHC) and clathrin light chain (CLC), across different lineages in Metamonada. Our data point to the loss of a bona fide CLC in the last Fornicata common ancestor (LFCA) with the emergence of a protein analogous to CLC (GlACLC) in the Giardia genus. Finally, the location of clathrin in the various compartments was quantified. Conclusions Taken together, this provides the first comprehensive nanometric view of Giardia’s endocytic system architecture and sheds light on the evolution of GlACLC analogues in the Fornicata supergroup and, specific to Giardia, as a possible adaptation to the formation and maintenance of stable clathrin assemblies at PVs. Supplementary Information The online version contains supplementary material available at 10.1186/s12915-022-01402-3.
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Affiliation(s)
- Rui Santos
- Institute of Parasitology, University of Zürich, Winterthurerstrasse 266a, 8057, Zürich, Switzerland.,Institute of Anatomy, University of Zürich, Winterthurerstrasse 190, 8057, Zürich, Switzerland
| | - Ásgeir Ástvaldsson
- Department of Cell and Molecular Biology, University of Uppsala, Husargatan 3, 752 37, Uppsala, Sweden.,Department of Microbiology, National Veterinary Institute, 751 23, Uppsala, Sweden
| | - Shweta V Pipaliya
- Division of Infectious Diseases, Department of Medicine, University of Alberta, Edmonton, Alberta, Canada.,School of Life Sciences, École Polytechnique Fédérale de Lausanne, Lausanne, Switzerland and Swiss Institute of Bioinformatics, Lausanne, Switzerland
| | - Jon Paulin Zumthor
- Amt für Lebensmittelsicherheit und Tiergesundheit Graubünden, Chur, Switzerland
| | - Joel B Dacks
- Division of Infectious Diseases, Department of Medicine, University of Alberta, Edmonton, Alberta, Canada.,Institute of Parasitology, Biology Centre, CAS, v.v.i., Branisovska 31, 370 05, Ceske Budejovice, Czech Republic
| | - Staffan Svärd
- Department of Cell and Molecular Biology, University of Uppsala, Husargatan 3, 752 37, Uppsala, Sweden
| | - Adrian B Hehl
- Institute of Parasitology, University of Zürich, Winterthurerstrasse 266a, 8057, Zürich, Switzerland
| | - Carmen Faso
- Institute of Cell Biology, University of Bern, Bern, Switzerland. .,Multidisciplinary Center for Infectious Diseases, Vetsuisse, University of Bern, Bern, Switzerland.
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18
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Yemets A, Plokhovska S, Pushkarova N, Blume Y. Quantum Dot-Antibody Conjugates for Immunofluorescence Studies of Biomolecules and Subcellular Structures. J Fluoresc 2022; 32:1713-1723. [PMID: 35670918 DOI: 10.1007/s10895-022-02968-5] [Citation(s) in RCA: 4] [Impact Index Per Article: 2.0] [Reference Citation Analysis] [Abstract] [Key Words] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Received: 01/24/2022] [Accepted: 05/05/2022] [Indexed: 01/14/2023]
Abstract
Quantum dots, or nanoscale semiconductors, are one of the most important materials for various research and development purposes. Due to their advantageous photoluminescence and electronic properties, namely, their unique photostability, high brightness, narrow emission spectra from visible to near-infrared wavelengths, convey them significant advantages over widely used fluorochromes, including organic dyes, fluorescent probes. Quantum dots are a unique instrument for a wide range of immunoassays with antibodies. The paper provides an overview of the developed and already applied methods of quantum dot surface modification, quantum dots conjugation to different antibodies (non-covalent, direct covalent linkage or with the use of special adapter molecules), as well as practical examples of recent quantum dot-antibody applications in the immunofluorescence microscopy for cell and cell structure imaging, fluorescent assays for biomolecules detection and in diagnostics of various diseases. The review presents advantages of quantum dot-antibody conjugation technology over the existing methods of immunofluorescence studies and a forward look into its potential prospects in biological and biomedical research.
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Affiliation(s)
- Alla Yemets
- Institute of Food Biotechnology and Genomics, National Academy of Sciences of Ukraine, Osypovskogo str., 2a, 04123, Kyiv, Ukraine.
| | - Svitlana Plokhovska
- Institute of Food Biotechnology and Genomics, National Academy of Sciences of Ukraine, Osypovskogo str., 2a, 04123, Kyiv, Ukraine
| | - Nadia Pushkarova
- Institute of Food Biotechnology and Genomics, National Academy of Sciences of Ukraine, Osypovskogo str., 2a, 04123, Kyiv, Ukraine
| | - Yaroslav Blume
- Institute of Food Biotechnology and Genomics, National Academy of Sciences of Ukraine, Osypovskogo str., 2a, 04123, Kyiv, Ukraine
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19
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Molina-Moreno M, González-Díaz I, Sicilia J, Crainiciuc G, Palomino-Segura M, Hidalgo A, Díaz-de-María F. ACME: Automatic feature extraction for cell migration examination through intravital microscopy imaging. Med Image Anal 2022; 77:102358. [DOI: 10.1016/j.media.2022.102358] [Citation(s) in RCA: 1] [Impact Index Per Article: 0.5] [Reference Citation Analysis] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Received: 06/23/2021] [Revised: 01/07/2022] [Accepted: 01/09/2022] [Indexed: 02/06/2023]
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20
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Reiche MA, Aaron JS, Boehm U, DeSantis MC, Hobson CM, Khuon S, Lee RM, Chew TL. When light meets biology - how the specimen affects quantitative microscopy. J Cell Sci 2022; 135:274812. [PMID: 35319069 DOI: 10.1242/jcs.259656] [Citation(s) in RCA: 10] [Impact Index Per Article: 5.0] [Reference Citation Analysis] [Abstract] [Key Words] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Indexed: 02/04/2023] Open
Abstract
Fluorescence microscopy images should not be treated as perfect representations of biology. Many factors within the biospecimen itself can drastically affect quantitative microscopy data. Whereas some sample-specific considerations, such as photobleaching and autofluorescence, are more commonly discussed, a holistic discussion of sample-related issues (which includes less-routine topics such as quenching, scattering and biological anisotropy) is required to appropriately guide life scientists through the subtleties inherent to bioimaging. Here, we consider how the interplay between light and a sample can cause common experimental pitfalls and unanticipated errors when drawing biological conclusions. Although some of these discrepancies can be minimized or controlled for, others require more pragmatic considerations when interpreting image data. Ultimately, the power lies in the hands of the experimenter. The goal of this Review is therefore to survey how biological samples can skew quantification and interpretation of microscopy data. Furthermore, we offer a perspective on how to manage many of these potential pitfalls.
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Affiliation(s)
- Michael A Reiche
- Advanced Imaging Center, Howard Hughes Medical Institute Janelia Research Campus, Ashburn, VA 20147, USA
| | - Jesse S Aaron
- Advanced Imaging Center, Howard Hughes Medical Institute Janelia Research Campus, Ashburn, VA 20147, USA
| | - Ulrike Boehm
- Advanced Imaging Center, Howard Hughes Medical Institute Janelia Research Campus, Ashburn, VA 20147, USA
| | - Michael C DeSantis
- Light Microscopy Facility, Howard Hughes Medical Institute Janelia Research Campus, Ashburn, VA 20147,USA
| | - Chad M Hobson
- Advanced Imaging Center, Howard Hughes Medical Institute Janelia Research Campus, Ashburn, VA 20147, USA
| | - Satya Khuon
- Advanced Imaging Center, Howard Hughes Medical Institute Janelia Research Campus, Ashburn, VA 20147, USA.,Howard Hughes Medical Institute Janelia Research Campus, Ashburn, VA 20147, USA
| | - Rachel M Lee
- Advanced Imaging Center, Howard Hughes Medical Institute Janelia Research Campus, Ashburn, VA 20147, USA
| | - Teng-Leong Chew
- Advanced Imaging Center, Howard Hughes Medical Institute Janelia Research Campus, Ashburn, VA 20147, USA.,Light Microscopy Facility, Howard Hughes Medical Institute Janelia Research Campus, Ashburn, VA 20147,USA
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21
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Watson ER, Taherian Fard A, Mar JC. Computational Methods for Single-Cell Imaging and Omics Data Integration. Front Mol Biosci 2022; 8:768106. [PMID: 35111809 PMCID: PMC8801747 DOI: 10.3389/fmolb.2021.768106] [Citation(s) in RCA: 3] [Impact Index Per Article: 1.5] [Reference Citation Analysis] [Abstract] [Key Words] [Track Full Text] [Download PDF] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Received: 09/14/2021] [Accepted: 11/29/2021] [Indexed: 12/12/2022] Open
Abstract
Integrating single cell omics and single cell imaging allows for a more effective characterisation of the underlying mechanisms that drive a phenotype at the tissue level, creating a comprehensive profile at the cellular level. Although the use of imaging data is well established in biomedical research, its primary application has been to observe phenotypes at the tissue or organ level, often using medical imaging techniques such as MRI, CT, and PET. These imaging technologies complement omics-based data in biomedical research because they are helpful for identifying associations between genotype and phenotype, along with functional changes occurring at the tissue level. Single cell imaging can act as an intermediary between these levels. Meanwhile new technologies continue to arrive that can be used to interrogate the genome of single cells and its related omics datasets. As these two areas, single cell imaging and single cell omics, each advance independently with the development of novel techniques, the opportunity to integrate these data types becomes more and more attractive. This review outlines some of the technologies and methods currently available for generating, processing, and analysing single-cell omics- and imaging data, and how they could be integrated to further our understanding of complex biological phenomena like ageing. We include an emphasis on machine learning algorithms because of their ability to identify complex patterns in large multidimensional data.
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Affiliation(s)
| | - Atefeh Taherian Fard
- Australian Institute for Bioengineering and Nanotechnology, The University of Queensland, Brisbane, QLD, Australia
| | - Jessica Cara Mar
- Australian Institute for Bioengineering and Nanotechnology, The University of Queensland, Brisbane, QLD, Australia
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22
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Aktar A, Wodz KM, Heit B. Monitoring Cellular Responses to Infection with Fluorescent Biosensors. Methods Mol Biol 2022; 2440:99-114. [PMID: 35218535 DOI: 10.1007/978-1-0716-2051-9_6] [Citation(s) in RCA: 0] [Impact Index Per Article: 0] [Reference Citation Analysis] [Abstract] [Key Words] [MESH Headings] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Indexed: 06/14/2023]
Abstract
Fluorescent biosensors are chemically or genetically encoded reporters of cellular processes, signaling pathways, or biomolecule concentration, whose output is quantified using fluorescence microscopy or fluorescence spectrometry. These biosensors can detect the target activity or metabolites via mechanisms including conversion between nonfluorescent and fluorescent forms, changes in reporter intensity, changes in the intensity ratio across fluorescence channels, alterations to the subcellular localization of the bioreporter, and by fluorescence resonance energy transfer. Here, we describe the use of a chemical photoconverting biosensor, and genetically encoded localization and ratiometric biosensors, for monitoring the cellular and signaling processes involved in pathogen-induced apoptosis and the resulting destruction of the pathogen. While this study uses biosensors to monitor responses to infection, these approaches can be readily translated to other cellular systems and other fluorescent biosensors.
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Affiliation(s)
- Amena Aktar
- Department of Microbiology and Immunology, Center for Human Immunology, The University of Western Ontario, London, ON, Canada
| | - Kasia M Wodz
- Department of Microbiology and Immunology, Center for Human Immunology, The University of Western Ontario, London, ON, Canada
| | - Bryan Heit
- Department of Microbiology and Immunology, Center for Human Immunology, The University of Western Ontario, London, ON, Canada.
- Robarts Research Institute, London, ON, Canada.
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23
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Grüneboom A, Aust O, Cibir Z, Weber F, Hermann DM, Gunzer M. Imaging innate immunity. Immunol Rev 2021; 306:293-303. [PMID: 34837251 DOI: 10.1111/imr.13048] [Citation(s) in RCA: 9] [Impact Index Per Article: 3.0] [Reference Citation Analysis] [Abstract] [Key Words] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Received: 09/29/2021] [Revised: 10/26/2021] [Accepted: 11/11/2021] [Indexed: 12/23/2022]
Abstract
Innate immunity is the first line of defense against infectious intruders and also plays a major role in the development of sterile inflammation. Direct microscopic imaging of the involved immune cells, especially neutrophil granulocytes, monocytes, and macrophages, has been performed since more than 150 years, and we still obtain novel insights on a frequent basis. Initially, intravital microscopy was limited to small-sized animal species, which were often invertebrates. In this review, we will discuss recent results on the biology of neutrophils and macrophages that have been obtained using confocal and two-photon microscopy of individual cells or subcellular structures as well as light-sheet microscopy of entire organs. This includes the role of these cells in infection defense and sterile inflammation in mammalian disease models relevant for human patients. We discuss their protective but also disease-enhancing activities during tumor growth and ischemia-reperfusion damage of the heart and brain. Finally, we provide two visions, one experimental and one applied, how our knowledge on the function of innate immune cells might be further enhanced and also be used in novel ways for disease diagnostics in the future.
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Affiliation(s)
- Anika Grüneboom
- Leibniz-Institut für Analytische Wissenschaften - ISAS - e.V, Dortmund, Germany
| | - Oliver Aust
- Leibniz-Institut für Analytische Wissenschaften - ISAS - e.V, Dortmund, Germany
| | - Zülal Cibir
- Institute for Experimental Immunology and Imaging, University Hospital, University Duisburg-Essen, Essen, Germany
| | - Flora Weber
- Leibniz-Institut für Analytische Wissenschaften - ISAS - e.V, Dortmund, Germany
| | - Dirk M Hermann
- Department of Neurology, University Hospital, University Duisburg-Essen, Essen, Germany
| | - Matthias Gunzer
- Leibniz-Institut für Analytische Wissenschaften - ISAS - e.V, Dortmund, Germany.,Institute for Experimental Immunology and Imaging, University Hospital, University Duisburg-Essen, Essen, Germany
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24
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Mukhamadiyarov RA, Bogdanov LA, Mishinov SV, Kutikhin AG. A Novel Technique for Preparation, Staining, and Visualization of Tissue with Metal Implants and Extraskeletal Calcification Areas. Sovrem Tekhnologii Med 2021; 12:13-20. [PMID: 34795988 PMCID: PMC8596281 DOI: 10.17691/stm2020.12.4.02] [Citation(s) in RCA: 1] [Impact Index Per Article: 0.3] [Reference Citation Analysis] [Abstract] [Key Words] [Track Full Text] [Download PDF] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Received: 09/11/2019] [Indexed: 11/27/2022] Open
Abstract
The aim of the study was to evaluate the efficacy of a novel technique for preparation, staining, and visualization of tissues containing extra-skeletal mineralization areas, all-metal implants or their prototypes for their subsequent examination using scanning electron microscopy in the backscattered electron mode.
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Affiliation(s)
- R A Mukhamadiyarov
- Senior Researcher, Laboratory for Fundamental Aspects of Atherosclerosis, Department of Experimental and Clinical Cardiology; Research Institute for Complex Issues of Cardiovascular Diseases, 6 Sosnovy Blvd, Kemerovo, 650002, Russia
| | - L A Bogdanov
- Junior Researcher, Laboratory for Fundamental Aspects of Atherosclerosis, Department of Experimental and Clinical Cardiology; Research Institute for Complex Issues of Cardiovascular Diseases, 6 Sosnovy Blvd, Kemerovo, 650002, Russia
| | - S V Mishinov
- Senior Researcher, Neurosurgeon, Neurosurgery Unit; Novosibirsk Scientific Research Institute of Traumatology and Orthopedics named after Ya.L. Tsivyan of the Ministry of Health of the Russian Federation, 17 Frunze St., Novosibirsk, 630091, Russia
| | - A G Kutikhin
- Head of the Laboratory for Fundamental Aspects of Atherosclerosis, Department of Experimental and Clinical Cardiology Research Institute for Complex Issues of Cardiovascular Diseases, 6 Sosnovy Blvd, Kemerovo, 650002, Russia
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25
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Mukhamadiyarov RA, Bogdanov LA, Glushkova TV, Shishkova DK, Kostyunin AE, Koshelev VA, Shabaev AR, Frolov AV, Stasev AN, Lyapin AA, Kutikhin AG. EMbedding and Backscattered Scanning Electron Microscopy: A Detailed Protocol for the Whole-Specimen, High-Resolution Analysis of Cardiovascular Tissues. Front Cardiovasc Med 2021; 8:739549. [PMID: 34760942 PMCID: PMC8573413 DOI: 10.3389/fcvm.2021.739549] [Citation(s) in RCA: 7] [Impact Index Per Article: 2.3] [Reference Citation Analysis] [Abstract] [Key Words] [Track Full Text] [Download PDF] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Received: 07/11/2021] [Accepted: 09/21/2021] [Indexed: 11/29/2022] Open
Abstract
Currently, an ultrastructural analysis of cardiovascular tissues is significantly complicated. Routine histopathological examinations and immunohistochemical staining suffer from a relatively low resolution of light microscopy, whereas the fluorescence imaging of plaques and bioprosthetic heart valves yields considerable background noise from the convoluted extracellular matrix that often results in a low signal-to-noise ratio. Besides, the sectioning of calcified or stent-expanded blood vessels or mineralised heart valves leads to a critical loss of their integrity, demanding other methods to be developed. Here, we designed a conceptually novel approach that combines conventional formalin fixation, sequential incubation in heavy metal solutions (osmium tetroxide, uranyl acetate or lanthanides, and lead citrate), and the embedding of the whole specimen into epoxy resin to retain its integrity while accessing the region of interest by grinding and polishing. Upon carbon sputtering, the sample is visualised by means of backscattered scanning electron microscopy. The technique fully preserves calcified and stent-expanded tissues, permits a detailed analysis of vascular and valvular composition and architecture, enables discrimination between multiple cell types (including endothelial cells, vascular smooth muscle cells, fibroblasts, adipocytes, mast cells, foam cells, foreign-body giant cells, canonical macrophages, neutrophils, and lymphocytes) and microvascular identities (arterioles, venules, and capillaries), and gives a technical possibility for quantitating the number, area, and density of the blood vessels. Hence, we suggest that our approach is capable of providing a pathophysiological insight into cardiovascular disease development. The protocol does not require specific expertise and can be employed in virtually any laboratory that has a scanning electron microscope.
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Affiliation(s)
- Rinat A Mukhamadiyarov
- Department of Experimental Medicine, Research Institute for Complex Issues of Cardiovascular Diseases, Kemerovo, Russia
| | - Leo A Bogdanov
- Department of Experimental Medicine, Research Institute for Complex Issues of Cardiovascular Diseases, Kemerovo, Russia
| | - Tatiana V Glushkova
- Department of Experimental Medicine, Research Institute for Complex Issues of Cardiovascular Diseases, Kemerovo, Russia
| | - Daria K Shishkova
- Department of Experimental Medicine, Research Institute for Complex Issues of Cardiovascular Diseases, Kemerovo, Russia
| | - Alexander E Kostyunin
- Department of Experimental Medicine, Research Institute for Complex Issues of Cardiovascular Diseases, Kemerovo, Russia
| | - Vladislav A Koshelev
- Department of Experimental Medicine, Research Institute for Complex Issues of Cardiovascular Diseases, Kemerovo, Russia
| | - Amin R Shabaev
- Department of Experimental Medicine, Research Institute for Complex Issues of Cardiovascular Diseases, Kemerovo, Russia
| | - Alexey V Frolov
- Department of Experimental Medicine, Research Institute for Complex Issues of Cardiovascular Diseases, Kemerovo, Russia
| | - Alexander N Stasev
- Department of Experimental Medicine, Research Institute for Complex Issues of Cardiovascular Diseases, Kemerovo, Russia
| | - Anton A Lyapin
- Department of Experimental Medicine, Research Institute for Complex Issues of Cardiovascular Diseases, Kemerovo, Russia
| | - Anton G Kutikhin
- Department of Experimental Medicine, Research Institute for Complex Issues of Cardiovascular Diseases, Kemerovo, Russia
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26
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Valli J, Sanderson J. Super-Resolution Fluorescence Microscopy Methods for Assessing Mouse Biology. Curr Protoc 2021; 1:e224. [PMID: 34436832 DOI: 10.1002/cpz1.224] [Citation(s) in RCA: 1] [Impact Index Per Article: 0.3] [Reference Citation Analysis] [Abstract] [Key Words] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Indexed: 12/16/2022]
Abstract
Super-resolution (diffraction unlimited) microscopy was developed 15 years ago; the developers were awarded the Nobel Prize in Chemistry in recognition of their work in 2014. Super-resolution microscopy is increasingly being applied to diverse scientific fields, from single molecules to cell organelles, viruses, bacteria, plants, and animals, especially the mammalian model organism Mus musculus. In this review, we explain how super-resolution microscopy, along with fluorescence microscopy from which it grew, has aided the renaissance of the light microscope. We cover experiment planning and specimen preparation and explain structured illumination microscopy, super-resolution radial fluctuations, stimulated emission depletion microscopy, single-molecule localization microscopy, and super-resolution imaging by pixel reassignment. The final section of this review discusses the strengths and weaknesses of each super-resolution technique and how to choose the best approach for your research. © 2021 The Authors. Current Protocols published by Wiley Periodicals LLC.
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Affiliation(s)
- Jessica Valli
- Edinburgh Super Resolution Imaging Consortium (ESRIC), Institute of Biological Chemistry, Biophysics and Bioengineering, Heriot-Watt University, Edinburgh, United Kingdom
| | - Jeremy Sanderson
- MRC Harwell Institute, Mammalian Genetics Unit, Harwell Campus, Oxfordshire, United Kingdom
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27
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Poole JJA, Mostaço-Guidolin LB. Optical Microscopy and the Extracellular Matrix Structure: A Review. Cells 2021; 10:1760. [PMID: 34359929 PMCID: PMC8308089 DOI: 10.3390/cells10071760] [Citation(s) in RCA: 19] [Impact Index Per Article: 6.3] [Reference Citation Analysis] [Abstract] [Key Words] [MESH Headings] [Grants] [Track Full Text] [Download PDF] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Received: 06/01/2021] [Revised: 07/07/2021] [Accepted: 07/09/2021] [Indexed: 02/07/2023] Open
Abstract
Biological tissues are not uniquely composed of cells. A substantial part of their volume is extracellular space, which is primarily filled by an intricate network of macromolecules constituting the extracellular matrix (ECM). The ECM serves as the scaffolding for tissues and organs throughout the body, playing an essential role in their structural and functional integrity. Understanding the intimate interaction between the cells and their structural microenvironment is central to our understanding of the factors driving the formation of normal versus remodelled tissue, including the processes involved in chronic fibrotic diseases. The visualization of the ECM is a key factor to track such changes successfully. This review is focused on presenting several optical imaging microscopy modalities used to characterize different ECM components. In this review, we describe and provide examples of applications of a vast gamut of microscopy techniques, such as widefield fluorescence, total internal reflection fluorescence, laser scanning confocal microscopy, multipoint/slit confocal microscopy, two-photon excited fluorescence (TPEF), second and third harmonic generation (SHG, THG), coherent anti-Stokes Raman scattering (CARS), fluorescence lifetime imaging microscopy (FLIM), structured illumination microscopy (SIM), stimulated emission depletion microscopy (STED), ground-state depletion microscopy (GSD), and photoactivated localization microscopy (PALM/fPALM), as well as their main advantages, limitations.
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Affiliation(s)
- Joshua J A Poole
- Department of Systems and Computer Engineering, Faculty of Engineering and Design, Carleton University 1125 Colonel By Drive, Ottawa, ON K1S 5B6, Canada
| | - Leila B Mostaço-Guidolin
- Department of Systems and Computer Engineering, Faculty of Engineering and Design, Carleton University 1125 Colonel By Drive, Ottawa, ON K1S 5B6, Canada
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28
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Chen X, Kandel ME, Popescu G. Spatial light interference microscopy: principle and applications to biomedicine. ADVANCES IN OPTICS AND PHOTONICS 2021; 13:353-425. [PMID: 35494404 PMCID: PMC9048520 DOI: 10.1364/aop.417837] [Citation(s) in RCA: 27] [Impact Index Per Article: 9.0] [Reference Citation Analysis] [Abstract] [Grants] [Track Full Text] [Subscribe] [Scholar Register] [Indexed: 05/03/2023]
Abstract
In this paper, we review spatial light interference microscopy (SLIM), a common-path, phase-shifting interferometer, built onto a phase-contrast microscope, with white-light illumination. As one of the most sensitive quantitative phase imaging (QPI) methods, SLIM allows for speckle-free phase reconstruction with sub-nanometer path-length stability. We first review image formation in QPI, scattering, and full-field methods. Then, we outline SLIM imaging from theory and instrumentation to diffraction tomography. Zernike's phase-contrast microscopy, phase retrieval in SLIM, and halo removal algorithms are discussed. Next, we discuss the requirements for operation, with a focus on software developed in-house for SLIM that enables high-throughput acquisition, whole slide scanning, mosaic tile registration, and imaging with a color camera. We introduce two methods for solving the inverse problem using SLIM, white-light tomography, and Wolf phase tomography. Lastly, we review the applications of SLIM in basic science and clinical studies. SLIM can study cell dynamics, cell growth and proliferation, cell migration, mass transport, etc. In clinical settings, SLIM can assist with cancer studies, reproductive technology, blood testing, etc. Finally, we review an emerging trend, where SLIM imaging in conjunction with artificial intelligence brings computational specificity and, in turn, offers new solutions to outstanding challenges in cell biology and pathology.
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29
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Chen R, Zhou H, Li A, Cheng X, Liu X, Huang F, Wang Y, Liu Y, Gong H, Liu X, Zeng S. Chemical Sectioning for Immunofluorescence Imaging. Anal Chem 2021; 93:8698-8703. [PMID: 34138541 DOI: 10.1021/acs.analchem.1c01702] [Citation(s) in RCA: 5] [Impact Index Per Article: 1.7] [Reference Citation Analysis] [Abstract] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Indexed: 11/30/2022]
Abstract
Immunofluorescence (IF) is a powerful investigative tool in biological research and medical diagnosis, whereas conventional imaging methods are always conflict between speed, contrast/resolution, and specimen volume. Chemical sectioning (CS) is an effective method to overcome the conflict, which works by chemically manipulating the off/on state of fluorescent materials and turning on only the extremely superficial surface fluorescence of tissues to realize the sectioning capacity of wide-field imaging. However, the current mechanism of CS is only applicable to samples labeled with pH-sensitive fluorescent proteins and still cannot fulfill samples immunolabeled with frequently used commercial fluorescent dyes. Here, immunofluorescence chemical sectioning (IF-CS) is described to present an off/on mechanism for Alexa dyes by complexation reactions, allowing CS imaging of IF labeled tissues. IF-CS enables IF freeing from out-of-focus interference in wide-field imaging and satisfying with multicolor imaging. IF-CS demonstrates the utility of the 3D submicron-resolution imaging of large immunolabeled tissues on the wide-field block-face system. IF-CS may remarkably facilitate systematic studies of refined subcellular architectures of endogenous proteins in intact biological systems.
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Affiliation(s)
- Ruixi Chen
- Britton Chance Center for Biomedical Photonics, Wuhan National Laboratory for Optoelectronics-Huazhong University of Science and Technology, Wuhan, Hubei 430074, China.,MoE Key Laboratory for Biomedical Photonics, Collaborative Innovation Center for Biomedical Engineering, School of Engineering Sciences, Huazhong University of Science and Technology, Wuhan, Hubei 430074, China
| | - Hongfu Zhou
- Britton Chance Center for Biomedical Photonics, Wuhan National Laboratory for Optoelectronics-Huazhong University of Science and Technology, Wuhan, Hubei 430074, China.,MoE Key Laboratory for Biomedical Photonics, Collaborative Innovation Center for Biomedical Engineering, School of Engineering Sciences, Huazhong University of Science and Technology, Wuhan, Hubei 430074, China
| | - Anan Li
- Britton Chance Center for Biomedical Photonics, Wuhan National Laboratory for Optoelectronics-Huazhong University of Science and Technology, Wuhan, Hubei 430074, China.,MoE Key Laboratory for Biomedical Photonics, Collaborative Innovation Center for Biomedical Engineering, School of Engineering Sciences, Huazhong University of Science and Technology, Wuhan, Hubei 430074, China
| | - Xiaofeng Cheng
- Britton Chance Center for Biomedical Photonics, Wuhan National Laboratory for Optoelectronics-Huazhong University of Science and Technology, Wuhan, Hubei 430074, China.,MoE Key Laboratory for Biomedical Photonics, Collaborative Innovation Center for Biomedical Engineering, School of Engineering Sciences, Huazhong University of Science and Technology, Wuhan, Hubei 430074, China
| | - Xiaoxiang Liu
- Britton Chance Center for Biomedical Photonics, Wuhan National Laboratory for Optoelectronics-Huazhong University of Science and Technology, Wuhan, Hubei 430074, China.,MoE Key Laboratory for Biomedical Photonics, Collaborative Innovation Center for Biomedical Engineering, School of Engineering Sciences, Huazhong University of Science and Technology, Wuhan, Hubei 430074, China
| | - Fei Huang
- Britton Chance Center for Biomedical Photonics, Wuhan National Laboratory for Optoelectronics-Huazhong University of Science and Technology, Wuhan, Hubei 430074, China.,MoE Key Laboratory for Biomedical Photonics, Collaborative Innovation Center for Biomedical Engineering, School of Engineering Sciences, Huazhong University of Science and Technology, Wuhan, Hubei 430074, China
| | - Yu Wang
- Britton Chance Center for Biomedical Photonics, Wuhan National Laboratory for Optoelectronics-Huazhong University of Science and Technology, Wuhan, Hubei 430074, China.,MoE Key Laboratory for Biomedical Photonics, Collaborative Innovation Center for Biomedical Engineering, School of Engineering Sciences, Huazhong University of Science and Technology, Wuhan, Hubei 430074, China
| | - Yurong Liu
- Britton Chance Center for Biomedical Photonics, Wuhan National Laboratory for Optoelectronics-Huazhong University of Science and Technology, Wuhan, Hubei 430074, China.,MoE Key Laboratory for Biomedical Photonics, Collaborative Innovation Center for Biomedical Engineering, School of Engineering Sciences, Huazhong University of Science and Technology, Wuhan, Hubei 430074, China
| | - Hui Gong
- Britton Chance Center for Biomedical Photonics, Wuhan National Laboratory for Optoelectronics-Huazhong University of Science and Technology, Wuhan, Hubei 430074, China.,MoE Key Laboratory for Biomedical Photonics, Collaborative Innovation Center for Biomedical Engineering, School of Engineering Sciences, Huazhong University of Science and Technology, Wuhan, Hubei 430074, China
| | - Xiuli Liu
- Britton Chance Center for Biomedical Photonics, Wuhan National Laboratory for Optoelectronics-Huazhong University of Science and Technology, Wuhan, Hubei 430074, China.,MoE Key Laboratory for Biomedical Photonics, Collaborative Innovation Center for Biomedical Engineering, School of Engineering Sciences, Huazhong University of Science and Technology, Wuhan, Hubei 430074, China
| | - Shaoqun Zeng
- Britton Chance Center for Biomedical Photonics, Wuhan National Laboratory for Optoelectronics-Huazhong University of Science and Technology, Wuhan, Hubei 430074, China.,MoE Key Laboratory for Biomedical Photonics, Collaborative Innovation Center for Biomedical Engineering, School of Engineering Sciences, Huazhong University of Science and Technology, Wuhan, Hubei 430074, China
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30
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Hellmuth KH, Sammaljärvi J, Siitari-Kauppi M, Robinet JC, Sardini P. STED nanoscopy - A novel way to image the pore space of geological materials. J Microsc 2021; 283:151-165. [PMID: 33895997 DOI: 10.1111/jmi.13016] [Citation(s) in RCA: 0] [Impact Index Per Article: 0] [Reference Citation Analysis] [Abstract] [Key Words] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Received: 12/11/2020] [Revised: 04/19/2021] [Accepted: 04/20/2021] [Indexed: 11/30/2022]
Abstract
STED nanoscopy (Stimulated Emission Depletion). which can resolve details far below the diffraction barrier has been applied hitherto preferentially to life sciences. The method is however also ideal for the investigation of geological matrices containing transparent minerals, an application tested here, to our knowledge, for the first time. The measurements on altered granitic rock and sedimentary clay rock, both containing very fine-grained phases, were conducted successfully. The STED fluorophore was dissolved in C-14-labelled methylmethacrylate (C-14-MMA) monomer which was polymerised within the rock matrix, thereby labelling the pore space in the geomaterials. Double labelling provided by the C-14-labelled MMA enables autoradiography and scanning electron microscopy (SEM), providing necessary complementary information for characterisation and quantification of porosity distributions and mineral and structure identification. Promising perspectives for further investigations of geological matrices by using different fluorophores and the optimisation of measuring procedures or even higher resolution are discussed. The combination of these different methods enlarges the observation scale of porosity from nanometre to centimetre scale.
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Affiliation(s)
| | | | | | | | - Paul Sardini
- IC2MP UMR CNRS 7285, HYDRASA, University of Poitiers, Poitiers, France
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31
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Imaging, Identification and Inhibition of Microorganisms Using AIEgens. Top Curr Chem (Cham) 2021; 379:21. [PMID: 33835299 DOI: 10.1007/s41061-021-00333-x] [Citation(s) in RCA: 1] [Impact Index Per Article: 0.3] [Reference Citation Analysis] [Abstract] [Key Words] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Received: 12/31/2020] [Accepted: 03/22/2021] [Indexed: 12/20/2022]
Abstract
Microorganisms, including bacteria, viruses and fungi, are ubiquitous in nature. Some are extremely beneficial to life on Earth, whereas some cause diseases and disrupt normal human physiology. Pathogenic microorganisms can also undergo mutations and develop resistance to antimicrobial agents, which complicates diagnostic and therapeutic regimens. This calls for continuing efforts to develop new strategies and tools that can provide fast, sensitive and accurate diagnosis, as well as effective treatment of ever-evolving infectious diseases. Aggregation-induced emission luminogens (AIEgens) have shown promise in imaging, identification and inhibition of various microbial species. Compared to conventional organic fluorophores, AIEgens can offer improved photostability, and have found utilities in imaging microorganisms. AIEgens have been shown to detect microbial viability and differentiate among different microbial strains. Theranostic AIEgens that integrate imaging and killing of microbes have also been developed. This review highlights examples in the literature where AIEgens have been employed as molecular probes in the imaging, discrimination and killing of bacteria, viruses and fungi.
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32
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Huang Q, Garrett A, Bose S, Blocker S, Rios AC, Clevers H, Shen X. The frontier of live tissue imaging across space and time. Cell Stem Cell 2021; 28:603-622. [PMID: 33798422 PMCID: PMC8034393 DOI: 10.1016/j.stem.2021.02.010] [Citation(s) in RCA: 23] [Impact Index Per Article: 7.7] [Reference Citation Analysis] [Abstract] [MESH Headings] [Grants] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Indexed: 02/07/2023]
Abstract
What you see is what you get-imaging techniques have long been essential for visualization and understanding of tissue development, homeostasis, and regeneration, which are driven by stem cell self-renewal and differentiation. Advances in molecular and tissue modeling techniques in the last decade are providing new imaging modalities to explore tissue heterogeneity and plasticity. Here we describe current state-of-the-art imaging modalities for tissue research at multiple scales, with a focus on explaining key tradeoffs such as spatial resolution, penetration depth, capture time/frequency, and moieties. We explore emerging tissue modeling and molecular tools that improve resolution, specificity, and throughput.
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Affiliation(s)
- Qiang Huang
- Department of Pediatric Surgery, Second Affiliated Hospital of Xi'an Jiaotong University, Xi'an, 710004 Shaanxi, China; Department of Biomedical Engineering, Pratt School of Engineering, Duke University, Durham, NC 27708, USA
| | - Aliesha Garrett
- Department of Biomedical Engineering, Pratt School of Engineering, Duke University, Durham, NC 27708, USA
| | - Shree Bose
- Department of Biomedical Engineering, Pratt School of Engineering, Duke University, Durham, NC 27708, USA
| | - Stephanie Blocker
- Center for In Vitro Microscopy, Duke University, Durham, NC 27708, USA
| | - Anne C Rios
- Princess Máxima Center for Pediatric Oncology, Utrecht 3584, the Netherlands; Department of Cancer Research, Oncode Institute, Hubrecht Institute-KNAW Utrecht, Utrecht 3584, the Netherlands
| | - Hans Clevers
- Princess Máxima Center for Pediatric Oncology, Utrecht 3584, the Netherlands; Department of Cancer Research, Oncode Institute, Hubrecht Institute-KNAW Utrecht, Utrecht 3584, the Netherlands; Hubrecht Institute, Royal Netherlands Academy of Arts and Sciences (KNAW) and University Medical Center (UMC) Utrecht, Utrecht 3584, the Netherlands
| | - Xiling Shen
- Department of Biomedical Engineering, Pratt School of Engineering, Duke University, Durham, NC 27708, USA.
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33
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Sacher WD, Chen FD, Moradi-Chameh H, Luo X, Fomenko A, Shah PT, Lordello T, Liu X, Almog IF, Straguzzi JN, Fowler TM, Jung Y, Hu T, Jeong J, Lozano AM, Lo PGQ, Valiante TA, Moreaux LC, Poon JKS, Roukes ML. Implantable photonic neural probes for light-sheet fluorescence brain imaging. NEUROPHOTONICS 2021; 8:025003. [PMID: 33898636 PMCID: PMC8059764 DOI: 10.1117/1.nph.8.2.025003] [Citation(s) in RCA: 17] [Impact Index Per Article: 5.7] [Reference Citation Analysis] [Abstract] [Key Words] [Track Full Text] [Subscribe] [Scholar Register] [Received: 08/12/2020] [Accepted: 03/04/2021] [Indexed: 05/07/2023]
Abstract
Significance: Light-sheet fluorescence microscopy (LSFM) is a powerful technique for high-speed volumetric functional imaging. However, in typical light-sheet microscopes, the illumination and collection optics impose significant constraints upon the imaging of non-transparent brain tissues. We demonstrate that these constraints can be surmounted using a new class of implantable photonic neural probes. Aim: Mass manufacturable, silicon-based light-sheet photonic neural probes can generate planar patterned illumination at arbitrary depths in brain tissues without any additional micro-optic components. Approach: We develop implantable photonic neural probes that generate light sheets in tissue. The probes were fabricated in a photonics foundry on 200-mm-diameter silicon wafers. The light sheets were characterized in fluorescein and in free space. The probe-enabled imaging approach was tested in fixed, in vitro, and in vivo mouse brain tissues. Imaging tests were also performed using fluorescent beads suspended in agarose. Results: The probes had 5 to 10 addressable sheets and average sheet thicknesses < 16 μ m for propagation distances up to 300 μ m in free space. Imaging areas were as large as ≈ 240 μ m × 490 μ m in brain tissue. Image contrast was enhanced relative to epifluorescence microscopy. Conclusions: The neural probes can lead to new variants of LSFM for deep brain imaging and experiments in freely moving animals.
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Affiliation(s)
- Wesley D. Sacher
- California Institute of Technology, Division of Physics, Mathematics, and Astronomy, Pasadena, California, United States
- Kavli Nanoscience Institute, California Institute of Technology, Pasadena, California, United States
- University of Toronto, Department of Electrical and Computer Engineering, Toronto, Ontario, Canada
- Max Planck Institute of Microstructure Physics, Halle, Germany
- Address all correspondence to Wesley D. Sacher, ; Michael L. Roukes,
| | - Fu-Der Chen
- University of Toronto, Department of Electrical and Computer Engineering, Toronto, Ontario, Canada
| | - Homeira Moradi-Chameh
- University Health Network, Krembil Research Institute, Division of Clinical and Computational Neuroscience, Toronto, Ontario, Canada
| | | | - Anton Fomenko
- University Health Network, Krembil Research Institute, Division of Clinical and Computational Neuroscience, Toronto, Ontario, Canada
| | - Prajay T. Shah
- University Health Network, Krembil Research Institute, Division of Clinical and Computational Neuroscience, Toronto, Ontario, Canada
| | - Thomas Lordello
- University of Toronto, Department of Electrical and Computer Engineering, Toronto, Ontario, Canada
| | - Xinyu Liu
- California Institute of Technology, Division of Physics, Mathematics, and Astronomy, Pasadena, California, United States
| | - Ilan Felts Almog
- University of Toronto, Department of Electrical and Computer Engineering, Toronto, Ontario, Canada
| | | | - Trevor M. Fowler
- California Institute of Technology, Division of Physics, Mathematics, and Astronomy, Pasadena, California, United States
| | - Youngho Jung
- University of Toronto, Department of Electrical and Computer Engineering, Toronto, Ontario, Canada
- Max Planck Institute of Microstructure Physics, Halle, Germany
| | - Ting Hu
- Agency for Science Technology and Research (A*STAR), Institute of Microelectronics, Singapore
| | - Junho Jeong
- University of Toronto, Department of Electrical and Computer Engineering, Toronto, Ontario, Canada
| | - Andres M. Lozano
- University Health Network, Krembil Research Institute, Division of Clinical and Computational Neuroscience, Toronto, Ontario, Canada
- University of Toronto, Toronto Western Hospital, Division of Neurosurgery, Department of Surgery, Toronto, Ontario, Canada
| | | | - Taufik A. Valiante
- University of Toronto, Department of Electrical and Computer Engineering, Toronto, Ontario, Canada
- University Health Network, Krembil Research Institute, Division of Clinical and Computational Neuroscience, Toronto, Ontario, Canada
- University of Toronto, Toronto Western Hospital, Division of Neurosurgery, Department of Surgery, Toronto, Ontario, Canada
- University of Toronto, Institute of Biomaterials and Biomedical Engineering, Toronto, Ontario, Canada
| | - Laurent C. Moreaux
- California Institute of Technology, Division of Physics, Mathematics, and Astronomy, Pasadena, California, United States
| | - Joyce K. S. Poon
- University of Toronto, Department of Electrical and Computer Engineering, Toronto, Ontario, Canada
- Max Planck Institute of Microstructure Physics, Halle, Germany
| | - Michael L. Roukes
- California Institute of Technology, Division of Physics, Mathematics, and Astronomy, Pasadena, California, United States
- Kavli Nanoscience Institute, California Institute of Technology, Pasadena, California, United States
- Address all correspondence to Wesley D. Sacher, ; Michael L. Roukes,
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Calvo V, Izquierdo M. Role of Actin Cytoskeleton Reorganization in Polarized Secretory Traffic at the Immunological Synapse. Front Cell Dev Biol 2021; 9:629097. [PMID: 33614660 PMCID: PMC7890359 DOI: 10.3389/fcell.2021.629097] [Citation(s) in RCA: 18] [Impact Index Per Article: 6.0] [Reference Citation Analysis] [Abstract] [Key Words] [Track Full Text] [Download PDF] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Received: 11/13/2020] [Accepted: 01/11/2021] [Indexed: 01/01/2023] Open
Abstract
T cell receptor (TCR) and B cell receptor (BCR) stimulation by antigen presented on an antigen-presenting cell (APC) induces the formation of the immune synapse (IS), the convergence of secretory vesicles from T and B lymphocytes toward the centrosome, and the polarization of the centrosome to the immune synapse. Immune synapse formation is associated with an initial increase in cortical F-actin at the synapse, followed by a decrease in F-actin density at the central region of the immune synapse, which contains the secretory domain. These reversible, actin cytoskeleton reorganization processes occur during lytic granule degranulation in cytotoxic T lymphocytes (CTL) and cytokine-containing vesicle secretion in T-helper (Th) lymphocytes. Recent evidences obtained in T and B lymphocytes forming synapses show that F-actin reorganization also occurs at the centrosomal area. F-actin reduction at the centrosomal area appears to be involved in centrosome polarization. In this review we deal with the biological significance of both cortical and centrosomal area F-actin reorganization and some of the derived biological consequences.
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Affiliation(s)
- Victor Calvo
- Departamento de Bioquímica, Facultad de Medicina, Instituto de Investigaciones Biomédicas Alberto Sols, Consejo Superior de Investigaciones Científicas - Universidad Autónoma de Madrid (CSIC-UAM), Madrid, Spain
| | - Manuel Izquierdo
- Instituto de Investigaciones Biomédicas Alberto Sols, Consejo Superior de Investigaciones Científicas - Universidad Autónoma de Madrid, Madrid, Spain
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35
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Cambré A, Aertsen A. Bacterial Vivisection: How Fluorescence-Based Imaging Techniques Shed a Light on the Inner Workings of Bacteria. Microbiol Mol Biol Rev 2020; 84:e00008-20. [PMID: 33115939 PMCID: PMC7599038 DOI: 10.1128/mmbr.00008-20] [Citation(s) in RCA: 12] [Impact Index Per Article: 3.0] [Reference Citation Analysis] [Abstract] [Key Words] [MESH Headings] [Grants] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Indexed: 12/11/2022] Open
Abstract
The rise in fluorescence-based imaging techniques over the past 3 decades has improved the ability of researchers to scrutinize live cell biology at increased spatial and temporal resolution. In microbiology, these real-time vivisections structurally changed the view on the bacterial cell away from the "watery bag of enzymes" paradigm toward the perspective that these organisms are as complex as their eukaryotic counterparts. Capitalizing on the enormous potential of (time-lapse) fluorescence microscopy and the ever-extending pallet of corresponding probes, initial breakthroughs were made in unraveling the localization of proteins and monitoring real-time gene expression. However, later it became clear that the potential of this technique extends much further, paving the way for a focus-shift from observing single events within bacterial cells or populations to obtaining a more global picture at the intra- and intercellular level. In this review, we outline the current state of the art in fluorescence-based vivisection of bacteria and provide an overview of important case studies to exemplify how to use or combine different strategies to gain detailed information on the cell's physiology. The manuscript therefore consists of two separate (but interconnected) parts that can be read and consulted individually. The first part focuses on the fluorescent probe pallet and provides a perspective on modern methodologies for microscopy using these tools. The second section of the review takes the reader on a tour through the bacterial cell from cytoplasm to outer shell, describing strategies and methods to highlight architectural features and overall dynamics within cells.
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Affiliation(s)
- Alexander Cambré
- KU Leuven, Department of Microbial and Molecular Systems, Faculty of Bioscience Engineering, Leuven, Belgium
| | - Abram Aertsen
- KU Leuven, Department of Microbial and Molecular Systems, Faculty of Bioscience Engineering, Leuven, Belgium
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36
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Parodi V, Jacchetti E, Osellame R, Cerullo G, Polli D, Raimondi MT. Nonlinear Optical Microscopy: From Fundamentals to Applications in Live Bioimaging. Front Bioeng Biotechnol 2020; 8:585363. [PMID: 33163482 PMCID: PMC7581943 DOI: 10.3389/fbioe.2020.585363] [Citation(s) in RCA: 35] [Impact Index Per Article: 8.8] [Reference Citation Analysis] [Abstract] [Key Words] [Track Full Text] [Download PDF] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Received: 07/20/2020] [Accepted: 09/16/2020] [Indexed: 12/13/2022] Open
Abstract
A recent challenge in the field of bioimaging is to image vital, thick, and complex tissues in real time and in non-invasive mode. Among the different tools available for diagnostics, nonlinear optical (NLO) multi-photon microscopy allows label-free non-destructive investigation of physio-pathological processes in live samples at sub-cellular spatial resolution, enabling to study the mechanisms underlying several cellular functions. In this review, we discuss the fundamentals of NLO microscopy and the techniques suitable for biological applications, such as two-photon excited fluorescence (TPEF), second and third harmonic generation (SHG-THG), and coherent Raman scattering (CRS). In addition, we present a few of the most recent examples of NLO imaging employed as a label-free diagnostic instrument to functionally monitor in vitro and in vivo vital biological specimens in their unperturbed state, highlighting the technological advantages of multi-modal, multi-photon NLO microscopy and the outstanding challenges in biomedical engineering applications.
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Affiliation(s)
- Valentina Parodi
- Department of Chemistry, Materials and Chemical Engineering “G. Natta”, Politecnico di Milano, Milan, Italy
| | - Emanuela Jacchetti
- Department of Chemistry, Materials and Chemical Engineering “G. Natta”, Politecnico di Milano, Milan, Italy
| | - Roberto Osellame
- Istituto di Fotonica e Nanotecnologie (IFN) – CNR, Milan, Italy
- Department of Physics, Politecnico di Milano, Milan, Italy
| | - Giulio Cerullo
- Istituto di Fotonica e Nanotecnologie (IFN) – CNR, Milan, Italy
- Department of Physics, Politecnico di Milano, Milan, Italy
| | - Dario Polli
- Istituto di Fotonica e Nanotecnologie (IFN) – CNR, Milan, Italy
- Department of Physics, Politecnico di Milano, Milan, Italy
| | - Manuela Teresa Raimondi
- Department of Chemistry, Materials and Chemical Engineering “G. Natta”, Politecnico di Milano, Milan, Italy
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37
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Keevend K, Coenen T, Herrmann IK. Correlative cathodoluminescence electron microscopy bioimaging: towards single protein labelling with ultrastructural context. NANOSCALE 2020; 12:15588-15603. [PMID: 32677648 DOI: 10.1039/d0nr02563a] [Citation(s) in RCA: 6] [Impact Index Per Article: 1.5] [Reference Citation Analysis] [Abstract] [MESH Headings] [Track Full Text] [Subscribe] [Scholar Register] [Indexed: 06/11/2023]
Abstract
The understanding of living systems and their building blocks relies heavily on the assessment of structure-function relationships at the nanoscale. Ever since the development of the first optical microscope, the reliance of scientists across disciplines on microscopy has increased. The development of the first electron microscope and with it the access to information at the nanoscale has prompted numerous disruptive discoveries. While fluorescence imaging allows identification of specific entities based on the labelling with fluorophores, the unlabelled constituents of the samples remain invisible. In electron microscopy on the other hand, structures can be comprehensively visualized based on their distinct electron density and geometry. Although electron microscopy is a powerful tool, it does not implicitly provide information on the location and activity of specific organic molecules. While correlative light and electron microscopy techniques have attempted to unify the two modalities, the resolution mismatch between the two data sets poses major challenges. Recent developments in optical super resolution microscopy enable high resolution correlative light and electron microscopy, however, with considerable constraints due to sample preparation requirements. Labelling of specific structures directly for electron microscopy using small gold nanoparticles (i.e. immunogold) has been used extensively. However, identification of specific entities solely based on electron contrast, and the differentiation from endogenous dense granules, remains challenging. Recently, the use of correlative cathodoluminescence electron microscopy (CCLEM) imaging based on luminescent inorganic nanocrystals has been proposed. While nanometric resolution can be reached for both the electron and the optical signal, high energy electron beams are potentially damaging to the sample. In this review, we discuss the opportunities of (volumetric) multi-color single protein labelling based on correlative cathodoluminescence electron microscopy, and its prospective impact on biomedical research in general. We elaborate on the potential challenges of correlative cathodoluminescence electron microscopy-based bioimaging and benchmark CCLEM against alternative high-resolution correlative imaging techniques.
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Affiliation(s)
- Kerda Keevend
- Laboratory for Particles Biology Interactions, Swiss Federal Laboratories for Materials Science and Technology (Empa), Lerchenfeldstrasse 5, CH-9014, St Gallen, Switzerland.
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38
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Murin CD. Considerations of Antibody Geometric Constraints on NK Cell Antibody Dependent Cellular Cytotoxicity. Front Immunol 2020; 11:1635. [PMID: 32849559 PMCID: PMC7406664 DOI: 10.3389/fimmu.2020.01635] [Citation(s) in RCA: 13] [Impact Index Per Article: 3.3] [Reference Citation Analysis] [Abstract] [Key Words] [MESH Headings] [Grants] [Track Full Text] [Download PDF] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Received: 04/18/2020] [Accepted: 06/18/2020] [Indexed: 12/31/2022] Open
Abstract
It has been well-established that antibody isotype, glycosylation, and epitope all play roles in the process of antibody dependent cellular cytotoxicity (ADCC). For natural killer (NK) cells, these phenotypes are linked to cellular activation through interaction with the IgG receptor FcγRIIIa, a single pass transmembrane receptor that participates in cytoplasmic signaling complexes. Therefore, it has been hypothesized that there may be underlying spatial and geometric principles that guide proper assembly of an activation complex within the NK cell immune synapse. Further, synergy of antibody phenotypic properties as well as allosteric changes upon antigen binding may also play an as-of-yet unknown role in ADCC. Understanding these facets, however, remains hampered by difficulties associated with studying immune synapse dynamics using classical approaches. In this review, I will discuss relevant NK cell biology related to ADCC, including the structural biology of Fc gamma receptors, and how the dynamics of the NK cell immune synapse are being studied using innovative microscopy techniques. I will provide examples from the literature demonstrating the effects of spatial and geometric constraints on the T cell receptor complex and how this relates to intracellular signaling and the molecular nature of lymphocyte activation complexes, including those of NK cells. Finally, I will examine how the integration of high-throughput and "omics" technologies will influence basic NK cell biology research moving forward. Overall, the goal of this review is to lay a basis for understanding the development of drugs and therapeutic antibodies aimed at augmenting appropriate NK cell ADCC activity in patients being treated for a wide range of illnesses.
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Affiliation(s)
- Charles D. Murin
- Department of Integrative Structural and Computational Biology, Scripps Research, La Jolla, CA, United States
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Schmidt AJ, Mayer JU, Wallace PK, Ronchese F, Price KM. Simultaneous Polychromatic Immunofluorescent Staining of Tissue Sections and Consecutive Imaging of up to Seven Parameters by Standard Confocal Microscopy. ACTA ACUST UNITED AC 2020; 91:e64. [PMID: 31763771 DOI: 10.1002/cpcy.64] [Citation(s) in RCA: 6] [Impact Index Per Article: 1.5] [Reference Citation Analysis] [Abstract] [Key Words] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Indexed: 11/11/2022]
Abstract
Confocal microscopy has been an important imaging tool for life scientists for over 20 years. Early techniques focused on indirect staining processes that involved staining with an unconjugated primary antibody, followed by incubation with a secondary fluorescent antibody that would reveal and amplify the signal of the primary antibody. With more and more directly conjugated fluorescent primary antibodies becoming commercially available, staining with multiple fluorescent primary antibodies is now more frequent. To date, staining with up to three primary antibodies and a nuclear dye is widely practiced. Here, we describe an important improvement to the standard polychromatic immunofluorescent staining protocol that allows the simultaneous detection of seven fluorescent parameters using a standard confocal laser scanning microscope with four laser lines and four photomultiplier tubes. By incorporating recently available tandem dyes that emit in the blue and violet regions of the visible light spectrum (Brilliant Blue and Brilliant Violet), we were able to differentiate several additional fluorochromes simultaneously. Due to the added complexity of 7-color immunofluorescent imaging, we developed a clear methodology to optimize antibody concentrations and simple guidelines on how to identify and correct non-specific signals. These are detailed in the following protocol. © 2019 by John Wiley & Sons, Inc. Basic Protocol: 7-Color immunofluorescent staining protocol using directly conjugated antibodies Support Protocol 1: Antibody titration protocol Support Protocol 2: Spillover optimization protocol.
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Affiliation(s)
| | | | - Paul K Wallace
- Department of Flow & Image Cytometry, Roswell Park Comprehensive Cancer Center, Buffalo, New York
| | - Franca Ronchese
- Malaghan Institute of Medical Research, Wellington, New Zealand
| | - Kylie M Price
- Malaghan Institute of Medical Research, Wellington, New Zealand
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Abstract
Optical imaging techniques are often used in neuroscience to understand brain function and discern disease pathogenesis. However, the optical diffraction limit precludes conventional optical imaging approaches from resolving nanoscopic structures with feature sizes smaller than 300 nm. Expansion microscopy (ExM) circumvents this limit by physically expanding preserved tissues embedded in a swellable hydrogel. Biomolecules of interest are covalently linked to a polymer matrix, which is then isotropically expanded at least 100-fold in size in pure water after mechanical homogenization of the tissue-gel. The sample can then be investigated with nanoscale precision using a conventional diffraction-limited microscope. The protocol described here is a variant of ExM that uses regents and equipment found in a typical biology laboratory and has been optimized for imaging proteins in expanded brain tissues. © 2019 by John Wiley & Sons, Inc. Basic Protocol: Expansion microscopy for intact brain tissue.
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Affiliation(s)
- Aleksandra Klimas
- Department of Biological Sciences, Carnegie Mellon University, Pittsburgh, Pennsylvania
| | - Brendan Gallagher
- Department of Biological Sciences, Carnegie Mellon University, Pittsburgh, Pennsylvania
| | - Yongxin Zhao
- Department of Biological Sciences, Carnegie Mellon University, Pittsburgh, Pennsylvania
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41
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Klimas A, Zhao Y. Expansion Microscopy: Toward Nanoscale Imaging of a Diverse Range of Biomolecules. ACS NANO 2020; 14:7689-7695. [PMID: 32628828 PMCID: PMC7456618 DOI: 10.1021/acsnano.0c04374] [Citation(s) in RCA: 5] [Impact Index Per Article: 1.3] [Reference Citation Analysis] [Abstract] [MESH Headings] [Grants] [Track Full Text] [Subscribe] [Scholar Register] [Indexed: 05/09/2023]
Abstract
Expansion microscopy (ExM) has become a powerful imaging tool for visualizing the nanoscale organization of protein and nucleic acid targets in cells and tissues using only a conventional microscope. Until recently, current ExM approaches have had limited applicability to imaging other biomolecules, such as lipids and small molecules. With the new TRITON probes reported by Wen et al. in this issue of ACS Nano, ExM can now be used to perform nanoscale imaging of the cytoskeleton and lipid membranes. In this Perspective, we offer a brief overview of recent developments in ExM, with a focus on biomolecule anchoring and labeling strategies that target a wide range of biomolecules to the water-swellable polymer formed in situ, a key step that ensures biomolecules or labels of interest are separated in space and can be resolved on a conventional microscope. In addition to these new advancements, we discuss challenges and future directions in this exciting field.
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Affiliation(s)
- Aleksandra Klimas
- Department of Biological Sciences, Carnegie Mellon University, Pittsburgh, PA, USA
| | - Yongxin Zhao
- Department of Biological Sciences, Carnegie Mellon University, Pittsburgh, PA, USA
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42
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Development of an Inverted Epifluorescence Microscope for Long-Term Monitoring of Bacteria in Multiplexed Microfluidic Devices. SENSORS 2020; 20:s20154140. [PMID: 32722401 PMCID: PMC7435752 DOI: 10.3390/s20154140] [Citation(s) in RCA: 2] [Impact Index Per Article: 0.5] [Reference Citation Analysis] [Abstract] [Key Words] [Track Full Text] [Download PDF] [Figures] [Subscribe] [Scholar Register] [Received: 06/23/2020] [Revised: 07/20/2020] [Accepted: 07/23/2020] [Indexed: 01/02/2023]
Abstract
Developing more efficient methods for antibiotic susceptibility testing is a pressing issue in novel drug development as bacterial resistance to antibiotics becomes increasingly common. Microfluidic devices have been demonstrated to be powerful platforms that allow researchers to perform multiplexed antibiotic testing. However, the level of multiplexing within microdevices is limited, evidencing the need of creating simple, low-cost and high-resolution imaging systems that can be integrated in antibiotic development pipelines. This paper describes the design and development of an epifluorescence inverted microscope that enables long-term monitoring of bacteria inside multiplexed microfluidic devices. The goal of this work is to provide a simple microscope powerful enough to allow single-cell analysis of bacteria at a reduced cost. This facilitates increasing the number of microscopes that are simultaneously used for antibiotic testing. We prove that the designed system is able to accurately detect fluorescent beads of 100 nm, demonstrating comparable features to high-end commercial microscopes and effectively achieving the resolution required for single-cell analysis of bacteria. The proposed microscope could thus increase the efficiency in antibiotic testing while reducing cost, size, weight, and power requirements, contributing to the successful development of new antibiotic drugs.
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43
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Jacquemet G, Carisey AF, Hamidi H, Henriques R, Leterrier C. The cell biologist's guide to super-resolution microscopy. J Cell Sci 2020; 133:133/11/jcs240713. [PMID: 32527967 DOI: 10.1242/jcs.240713] [Citation(s) in RCA: 74] [Impact Index Per Article: 18.5] [Reference Citation Analysis] [Abstract] [Key Words] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Indexed: 12/22/2022] Open
Abstract
Fluorescence microscopy has become a ubiquitous method to observe the location of specific molecular components within cells. However, the resolution of light microscopy is limited by the laws of diffraction to a few hundred nanometers, blurring most cellular details. Over the last two decades, several techniques - grouped under the 'super-resolution microscopy' moniker - have been designed to bypass this limitation, revealing the cellular organization down to the nanoscale. The number and variety of these techniques have steadily increased, to the point that it has become difficult for cell biologists and seasoned microscopists alike to identify the specific technique best suited to their needs. Available techniques include image processing strategies that generate super-resolved images, optical imaging schemes that overcome the diffraction limit and sample manipulations that expand the size of the biological sample. In this Cell Science at a Glance article and the accompanying poster, we provide key pointers to help users navigate through the various super-resolution methods by briefly summarizing the principles behind each technique, highlighting both critical strengths and weaknesses, as well as providing example images.
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Affiliation(s)
- Guillaume Jacquemet
- Turku Bioscience Centre, University of Turku and Åbo Akademi University, FI-20520 Turku, Finland .,Faculty of Science and Engineering, Cell Biology, Åbo Akademi University, 20520 Turku, Finland
| | - Alexandre F Carisey
- William T. Shearer Center for Human Immunobiology, Baylor College of Medicine and Texas Children's Hospital, 1102 Bates Street, Houston 77030 TX, USA
| | - Hellyeh Hamidi
- Turku Bioscience Centre, University of Turku and Åbo Akademi University, FI-20520 Turku, Finland
| | - Ricardo Henriques
- University College London, London WC1E 6BT, UK .,The Francis Crick Institute, London NW1 1AT, UK
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Abstract
The light (or optical) microscope is the icon of science. The aphorism "seeing is believing" is often quoted in scientific papers involving microscopy. Unlike many scientific instruments, the light microscope will deliver an image however badly it is set up. Fluorescence microscopy is a widely used research tool across all disciplines of biological and biomedical science. Most universities and research institutions have microscopes, including confocal microscopes. This introductory paper in a series detailing advanced light microscopy techniques explains the foundations of both electron and light microscopy for biologists and life scientists working with the mouse. An explanation is given of how an image is formed. A description is given of how to set up a light microscope, whether it be a brightfield light microscope on the laboratory bench, a widefield fluorescence microscope, or a confocal microscope. These explanations are accompanied by operational protocols. A full explanation on how to set up and adjust a microscope according to the principles of Köhler illumination is given. The importance of Nyquist sampling is discussed. Guidelines are given on how to choose the best microscope to image the particular sample or slide preparation that you are working with. These are the basic principles of microscopy that a researcher must have an understanding of when operating core bioimaging facility instruments, in order to collect high-quality images. © 2020 The Authors. Basic Protocol 1: Setting up Köhler illumination for a brightfield microscope Basic Protocol 2: Aligning the fluorescence bulb and setting up Köhler illumination for a widefield fluorescence microscope Basic Protocol 3: Generic protocol for operating a confocal microscope.
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Affiliation(s)
- Jeremy Sanderson
- Bioimaging Facility Manager, MRC Harwell Institute, Mammalian Genetics Unit, Harwell Campus, Oxfordshire, UK
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45
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McKinley KL, Castillo-Azofeifa D, Klein OD. Tools and Concepts for Interrogating and Defining Cellular Identity. Cell Stem Cell 2020; 26:632-656. [PMID: 32386555 PMCID: PMC7250495 DOI: 10.1016/j.stem.2020.03.015] [Citation(s) in RCA: 19] [Impact Index Per Article: 4.8] [Reference Citation Analysis] [Abstract] [Key Words] [MESH Headings] [Grants] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Indexed: 12/22/2022]
Abstract
Defining the mechanisms that generate specialized cell types and coordinate their functions is critical for understanding organ development and renewal. New tools and discoveries are challenging and refining our definitions of a cell type. A rapidly growing toolkit for single-cell analyses has expanded the number of markers that can be assigned to a cell simultaneously, revealing heterogeneity within cell types that were previously regarded as homogeneous populations. Additionally, cell types defined by specific molecular markers can exhibit distinct, context-dependent functions; for example, between tissues in homeostasis and those responding to damage. Here we review the current technologies used to identify and characterize cells, and we discuss how experimental and pathological perturbations are adding increasing complexity to our definitions of cell identity.
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Affiliation(s)
- Kara L McKinley
- Department of Cellular and Molecular Pharmacology, University of California, San Francisco, San Francisco, CA, USA
| | - David Castillo-Azofeifa
- Department of Orofacial Sciences, University of California, San Francisco, San Francisco, CA, USA; Program in Craniofacial Biology, University of California, San Francisco, San Francisco, CA, USA
| | - Ophir D Klein
- Department of Orofacial Sciences, University of California, San Francisco, San Francisco, CA, USA; Program in Craniofacial Biology, University of California, San Francisco, San Francisco, CA, USA; Department of Pediatrics, University of California, San Francisco, San Francisco, CA, USA; Institute for Human Genetics, University of California, San Francisco, San Francisco, CA, USA.
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46
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Marquez A, Gómez-Fontela M, Lauzurica S, Candorcio-Simón R, Munoz-Martin D, Morales M, Ubago M, Toledo C, Lauzurica P, Molpeceres C. Fluorescence enhanced BA-LIFT for single cell detection and isolation. Biofabrication 2020; 12:025019. [DOI: 10.1088/1758-5090/ab6138] [Citation(s) in RCA: 12] [Impact Index Per Article: 3.0] [Reference Citation Analysis] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Indexed: 01/17/2023]
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47
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Zdańkowski P, Trusiak M, McGloin D, Swedlow JR. Numerically Enhanced Stimulated Emission Depletion Microscopy with Adaptive Optics for Deep-Tissue Super-Resolved Imaging. ACS NANO 2020; 14:394-405. [PMID: 31841303 DOI: 10.1021/acsnano.9b05891] [Citation(s) in RCA: 5] [Impact Index Per Article: 1.3] [Reference Citation Analysis] [Abstract] [Key Words] [MESH Headings] [Track Full Text] [Subscribe] [Scholar Register] [Indexed: 05/19/2023]
Abstract
In stimulated emission depletion (STED) nanoscopy, the major origin of decreased signal-to-noise ratio within images can be attributed to sample photobleaching and strong optical aberrations. This is due to STED utilizing a high-power depletion laser (increasing the risk of photodamage), while the depletion beam is very sensitive to sample-induced aberrations. Here, we demonstrate a custom-built STED microscope with automated aberration correction that is capable of 3D super-resolution imaging through thick, highly aberrating tissue. We introduce and investigate a state of the art image denoising method by block-matching and collaborative 3D filtering (BM3D) to numerically enhance fine object details otherwise mixed with noise and further enhance the image quality. Numerical denoising provides an increase in the final effective resolution of the STED imaging of 31% using the well established Fourier ring correlation metric. Results achieved through the combination of aberration correction and tailored image processing are experimentally validated through super-resolved 3D imaging of axons in differentiated induced pluripotent stem cells growing under an 80 μm thick layer of tissue with lateral and axial resolution of 204 and 310 nm, respectively.
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Affiliation(s)
- Piotr Zdańkowski
- Centre for Gene Regulation and Expression, School of Life Sciences , University of Dundee , Dundee DD1 5EH , United Kingdom
- SUPA, School of Science and Engineering , University of Dundee , Dundee DD1 4HN , United Kingdom
- Institute of Micromechanics and Photonics , Warsaw University of Technology , 8 A. Boboli Street , Warsaw 02-525 , Poland
| | - Maciej Trusiak
- Institute of Micromechanics and Photonics , Warsaw University of Technology , 8 A. Boboli Street , Warsaw 02-525 , Poland
| | - David McGloin
- SUPA, School of Science and Engineering , University of Dundee , Dundee DD1 4HN , United Kingdom
- School of Electrical and Data Engineering , University of Technology Sydney , Ultimo , New South Wales 2007 , Australia
| | - Jason R Swedlow
- Centre for Gene Regulation and Expression, School of Life Sciences , University of Dundee , Dundee DD1 5EH , United Kingdom
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48
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Liu SL, Wang ZG, Xie HY, Liu AA, Lamb DC, Pang DW. Single-Virus Tracking: From Imaging Methodologies to Virological Applications. Chem Rev 2020; 120:1936-1979. [PMID: 31951121 PMCID: PMC7075663 DOI: 10.1021/acs.chemrev.9b00692] [Citation(s) in RCA: 110] [Impact Index Per Article: 27.5] [Reference Citation Analysis] [Abstract] [Track Full Text] [Download PDF] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Indexed: 12/23/2022]
Abstract
![]()
Uncovering
the mechanisms of virus infection and assembly is crucial
for preventing the spread of viruses and treating viral disease. The
technique of single-virus tracking (SVT), also known as single-virus
tracing, allows one to follow individual viruses at different parts
of their life cycle and thereby provides dynamic insights into fundamental
processes of viruses occurring in live cells. SVT is typically based
on fluorescence imaging and reveals insights into previously unreported
infection mechanisms. In this review article, we provide the readers
a broad overview of the SVT technique. We first summarize recent advances
in SVT, from the choice of fluorescent labels and labeling strategies
to imaging implementation and analytical methodologies. We then describe
representative applications in detail to elucidate how SVT serves
as a valuable tool in virological research. Finally, we present our
perspectives regarding the future possibilities and challenges of
SVT.
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Affiliation(s)
- Shu-Lin Liu
- State Key Laboratory of Medicinal Chemical Biology, Tianjin Key Laboratory of Biosensing and Molecular Recognition, Research Center for Analytical Sciences, College of Chemistry, and School of Medicine , Nankai University , Tianjin 300071 , P. R. China.,Engineering Research Center of Nano-Geomaterials of Ministry of Education, Faculty of Materials Science and Chemistry , China University of Geosciences , Wuhan 430074 , P. R. China
| | - Zhi-Gang Wang
- State Key Laboratory of Medicinal Chemical Biology, Tianjin Key Laboratory of Biosensing and Molecular Recognition, Research Center for Analytical Sciences, College of Chemistry, and School of Medicine , Nankai University , Tianjin 300071 , P. R. China
| | - Hai-Yan Xie
- School of Life Science , Beijing Institute of Technology , Beijing 100081 , P. R. China
| | - An-An Liu
- State Key Laboratory of Medicinal Chemical Biology, Tianjin Key Laboratory of Biosensing and Molecular Recognition, Research Center for Analytical Sciences, College of Chemistry, and School of Medicine , Nankai University , Tianjin 300071 , P. R. China
| | - Don C Lamb
- Physical Chemistry, Department of Chemistry, Center for Nanoscience (CeNS), and Center for Integrated Protein Science Munich (CIPSM) and Nanosystems Initiative Munich (NIM) , Ludwig-Maximilians-Universität , München , 81377 , Germany
| | - Dai-Wen Pang
- State Key Laboratory of Medicinal Chemical Biology, Tianjin Key Laboratory of Biosensing and Molecular Recognition, Research Center for Analytical Sciences, College of Chemistry, and School of Medicine , Nankai University , Tianjin 300071 , P. R. China.,College of Chemistry and Molecular Sciences, State Key Laboratory of Virology, The Institute for Advanced Studies, and Wuhan Institute of Biotechnology , Wuhan University , Wuhan 430072 , P. R. China
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Chen H, Yang P, Li Y, Zhang L, Ding F, He X, Shen J. Insight into triphenylamine and coumarin serving as copper (II) sensors with "OFF" strategy and for bio-imaging in living cells. SPECTROCHIMICA ACTA. PART A, MOLECULAR AND BIOMOLECULAR SPECTROSCOPY 2020; 224:117384. [PMID: 31336321 DOI: 10.1016/j.saa.2019.117384] [Citation(s) in RCA: 20] [Impact Index Per Article: 5.0] [Reference Citation Analysis] [Abstract] [Key Words] [MESH Headings] [Track Full Text] [Subscribe] [Scholar Register] [Received: 05/06/2019] [Revised: 07/10/2019] [Accepted: 07/12/2019] [Indexed: 06/10/2023]
Abstract
Chemosensing is one of the widest and powerful techniques for response to anions and cations in living systems serving as bio-probes. Meanwhile, copper(II) (Cu(II)) widely exists in the environment and the human body as a common trace element, which plays an necessary role in most physiological processes. Thus, it is extremely urgent to explore means for effective, rapid and convenient detection of Cu(II) in living cells. Herein, we introduce a novel strategy for designing triphenylamine (TS) and coumarin-based (CS) functional sensors for Cu(II) detection with fluorescence "OFF" switching mechanism by blocking intramolecular charge transfer (ICT). Based on this design strategy, we have demonstrated two kinds of fluorophores sensors with aunique new fluorescent dye and excellent photophysical properties, which have shown rapid recognition of Cu(II) via a stoichiometric ratio of 2:1 and the proposed binding mode was confirmed by the single-crystal structure of CS-Cu(II) complex. In addition, we have carried out density functional theory (DFT) calculation with the B3LYP exchange functional employing RB3LYP/6-31G basis sets to get insight into the mechanism of Cu(II)-sensors alongside their optical properties. Furthermore, the sensors were capable of bio-imaging Cu(II) in living cancer cells (HepG2, A549 and Hela) with low cytotoxicity and good biocompatibility shown. Taken together, We expect that this novel strategy would provide new insight into the development of Cu(II) detection techniques and could be used more for biomedical applications.
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Affiliation(s)
- Hong Chen
- School of Ophthalmology & Optometry, School of Biomedical Engineering, Wenzhou Medical University, Wenzhou, Zhejiang 325035, China; Luoyang Key Laboratory of Organic Functional Molecules, College of Food and Drug, Luoyang Normal University, Luoyang, Henan 471934, China
| | - Ping Yang
- State Key Laboratory of Applied Microbiology Southern China, Guangdong Provincial Key Laboratory of Microbial Culture Collection and Application, Guangdong Open Laboratory of Applied Microbiology, Guangdong Institute of Microbiology, Guangzhou 510070, China
| | - Yahui Li
- School of Ophthalmology & Optometry, School of Biomedical Engineering, Wenzhou Medical University, Wenzhou, Zhejiang 325035, China
| | - Lilei Zhang
- College of Chemistry and Chemical Engineering, Luoyang Normal University, Luoyang, Henan 471934, China
| | - Feng Ding
- Department of Microbiology & Immunology, School of Basic Medical Sciences, Wenzhou Medical University, Wenzhou, Zhejiang 325035, China
| | - Xiaojun He
- School of Ophthalmology & Optometry, School of Biomedical Engineering, Wenzhou Medical University, Wenzhou, Zhejiang 325035, China
| | - Jianliang Shen
- School of Ophthalmology & Optometry, School of Biomedical Engineering, Wenzhou Medical University, Wenzhou, Zhejiang 325035, China; Wenzhou Institute of Biomaterials and Engineering, Chinese Academy of Science, Wenzhou, Zhejiang 325001, China.
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Glancy B. Visualizing Mitochondrial Form and Function within the Cell. Trends Mol Med 2020; 26:58-70. [PMID: 31706841 PMCID: PMC6938546 DOI: 10.1016/j.molmed.2019.09.009] [Citation(s) in RCA: 48] [Impact Index Per Article: 12.0] [Reference Citation Analysis] [Abstract] [Key Words] [MESH Headings] [Grants] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Received: 08/14/2019] [Revised: 09/25/2019] [Accepted: 09/25/2019] [Indexed: 12/12/2022]
Abstract
The specific cellular role of mitochondria is influenced by the surrounding environment because effective mitochondrial function requires the delivery of inputs (e.g., oxygen) and export of products (e.g., signaling molecules) to and from other cellular components, respectively. Recent technological developments in mitochondrial imaging have led to a more precise and comprehensive understanding of the spatial relationships governing the function of this complex organelle, opening a new era of mitochondrial research. Here, I highlight current imaging approaches for visualizing mitochondrial form and function within complex cellular environments. Increasing clarity of mitochondrial behavior within cells will continue to lend mechanistic insights into the role of mitochondria under normal and pathological conditions and point to spatially regulated processes that can be targeted to improve cellular function.
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Affiliation(s)
- Brian Glancy
- National Heart, Lung, and Blood Institute, National Institutes of Health, Bethesda, MD, USA; National Institute of Arthritis and Musculoskeletal and Skin Diseases, National Institutes of Health, Bethesda, MD, USA.
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