1
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Lautenschläger J, Wagner-Valladolid S, Stephens AD, Fernández-Villegas A, Hockings C, Mishra A, Manton JD, Fantham MJ, Lu M, Rees EJ, Kaminski CF, Kaminski Schierle GS. Intramitochondrial proteostasis is directly coupled to α-synuclein and amyloid β1-42 pathologies. J Biol Chem 2020; 295:10138-10152. [PMID: 32385113 PMCID: PMC7383368 DOI: 10.1074/jbc.ra119.011650] [Citation(s) in RCA: 18] [Impact Index Per Article: 4.5] [Reference Citation Analysis] [Abstract] [Key Words] [MESH Headings] [Grants] [Track Full Text] [Download PDF] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Received: 10/27/2019] [Revised: 04/30/2020] [Indexed: 12/16/2022] Open
Abstract
Mitochondrial dysfunction has long been implicated in the neurodegenerative disorder Parkinson's disease (PD); however, it is unclear how mitochondrial impairment and α-synuclein pathology are coupled. Using specific mitochondrial inhibitors, EM analysis, and biochemical assays, we report here that intramitochondrial protein homeostasis plays a major role in α-synuclein aggregation. We found that interference with intramitochondrial proteases, such as HtrA2 and Lon protease, and mitochondrial protein import significantly aggravates α-synuclein seeding. In contrast, direct inhibition of mitochondrial complex I, an increase in intracellular calcium concentration, or formation of reactive oxygen species, all of which have been associated with mitochondrial stress, did not affect α-synuclein pathology. We further demonstrate that similar mechanisms are involved in amyloid-β 1-42 (Aβ42) aggregation. Our results suggest that, in addition to other protein quality control pathways, such as the ubiquitin-proteasome system, mitochondria per se can influence protein homeostasis of cytosolic aggregation-prone proteins. We propose that approaches that seek to maintain mitochondrial fitness, rather than target downstream mitochondrial dysfunction, may aid in the search for therapeutic strategies to manage PD and related neuropathologies.
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Affiliation(s)
- Janin Lautenschläger
- Molecular Neuroscience Group, Department of Chemical Engineering and Biotechnology, University of Cambridge, West Cambridge Site, Philippa Fawcett Drive, Cambridge, United Kingdom ;
| | - Sara Wagner-Valladolid
- Molecular Neuroscience Group, Department of Chemical Engineering and Biotechnology, University of Cambridge, West Cambridge Site, Philippa Fawcett Drive, Cambridge, United Kingdom
| | - Amberley D Stephens
- Molecular Neuroscience Group, Department of Chemical Engineering and Biotechnology, University of Cambridge, West Cambridge Site, Philippa Fawcett Drive, Cambridge, United Kingdom
| | - Ana Fernández-Villegas
- Molecular Neuroscience Group, Department of Chemical Engineering and Biotechnology, University of Cambridge, West Cambridge Site, Philippa Fawcett Drive, Cambridge, United Kingdom
| | - Colin Hockings
- Molecular Neuroscience Group, Department of Chemical Engineering and Biotechnology, University of Cambridge, West Cambridge Site, Philippa Fawcett Drive, Cambridge, United Kingdom
| | - Ajay Mishra
- Molecular Neuroscience Group, Department of Chemical Engineering and Biotechnology, University of Cambridge, West Cambridge Site, Philippa Fawcett Drive, Cambridge, United Kingdom
| | - James D Manton
- Quantitative Imaging Group, Department of Chemical Engineering and Biotechnology, University of Cambridge, West Cambridge Site, Philippa Fawcett Drive, Cambridge, United Kingdom
| | - Marcus J Fantham
- Laser Analytics Group, Department of Chemical Engineering and Biotechnology, University of Cambridge, West Cambridge Site, Philippa Fawcett Drive, Cambridge, United Kingdom
| | - Meng Lu
- Molecular Neuroscience Group, Department of Chemical Engineering and Biotechnology, University of Cambridge, West Cambridge Site, Philippa Fawcett Drive, Cambridge, United Kingdom
| | - Eric J Rees
- Quantitative Imaging Group, Department of Chemical Engineering and Biotechnology, University of Cambridge, West Cambridge Site, Philippa Fawcett Drive, Cambridge, United Kingdom
| | - Clemens F Kaminski
- Laser Analytics Group, Department of Chemical Engineering and Biotechnology, University of Cambridge, West Cambridge Site, Philippa Fawcett Drive, Cambridge, United Kingdom
| | - Gabriele S Kaminski Schierle
- Molecular Neuroscience Group, Department of Chemical Engineering and Biotechnology, University of Cambridge, West Cambridge Site, Philippa Fawcett Drive, Cambridge, United Kingdom ;
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2
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Bielec K, Bubak G, Kalwarczyk T, Holyst R. Analysis of Brightness of a Single Fluorophore for Quantitative Characterization of Biochemical Reactions. J Phys Chem B 2020; 124:1941-1948. [PMID: 32059107 PMCID: PMC7497653 DOI: 10.1021/acs.jpcb.0c00770] [Citation(s) in RCA: 9] [Impact Index Per Article: 2.3] [Reference Citation Analysis] [Abstract] [Track Full Text] [Download PDF] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Indexed: 01/08/2023]
Abstract
![]()
Intrinsic
molecular brightness (MB) is a number of emitted photons
per second per molecule. When a substrate labeled by a fluorophore
and a second unlabeled substrate form a complex in solution, the MB
of the fluorophore changes. Here we use this change to determine the equilibrium constant (K) for the formation of the complex at pM concentrations.
To illustrate this method, we used a reaction of DNA hybridization,
where only one of the strands was fluorescently labeled. We determined K at the substrate concentrations from 80 pM to 30 nM. We
validated this method against Förster resonance energy transfer
(FRET). This method is much simpler than FRET as it requires only
one fluorophore in the complex with a very small (a f̃ew percent)
change in MB.
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Affiliation(s)
- Krzysztof Bielec
- Institute of Physical Chemistry, Polish Academy of Sciences, Kasprzaka 44/52, 01-224 Warsaw, Poland
| | - Grzegorz Bubak
- Institute of Physical Chemistry, Polish Academy of Sciences, Kasprzaka 44/52, 01-224 Warsaw, Poland
| | - Tomasz Kalwarczyk
- Institute of Physical Chemistry, Polish Academy of Sciences, Kasprzaka 44/52, 01-224 Warsaw, Poland
| | - Robert Holyst
- Institute of Physical Chemistry, Polish Academy of Sciences, Kasprzaka 44/52, 01-224 Warsaw, Poland
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3
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Laine RF, Sinnige T, Ma KY, Haack AJ, Poudel C, Gaida P, Curry N, Perni M, Nollen EA, Dobson CM, Vendruscolo M, Kaminski Schierle GS, Kaminski CF. Fast Fluorescence Lifetime Imaging Reveals the Aggregation Processes of α-Synuclein and Polyglutamine in Aging Caenorhabditis elegans. ACS Chem Biol 2019; 14:1628-1636. [PMID: 31246415 PMCID: PMC7612977 DOI: 10.1021/acschembio.9b00354] [Citation(s) in RCA: 23] [Impact Index Per Article: 4.6] [Reference Citation Analysis] [Abstract] [MESH Headings] [Grants] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Indexed: 12/17/2022]
Abstract
The nematode worm Caenorhabditis elegans has emerged as an important model organism in the study of the molecular mechanisms of protein misfolding diseases associated with amyloid formation because of its small size, ease of genetic manipulation, and optical transparency. Obtaining a reliable and quantitative read-out of protein aggregation in this system, however, remains a challenge. To address this problem, we here present a fast time-gated fluorescence lifetime imaging (TG-FLIM) method and show that it provides functional insights into the process of protein aggregation in living animals by enabling the rapid characterization of different types of aggregates. Specifically, in longitudinal studies of C. elegans models of Parkinson's and Huntington's diseases, we observed marked differences in the aggregation kinetics and the nature of the protein inclusions formed by α-synuclein and polyglutamine. In particular, we found that α-synuclein inclusions do not display amyloid-like features until late in the life of the worms, whereas polyglutamine forms amyloid characteristics rapidly in early adulthood. Furthermore, we show that the TG-FLIM method is capable of imaging live and non-anaesthetized worms moving in specially designed agarose microchambers. Taken together, our results show that the TG-FLIM method enables high-throughput functional imaging of living C. elegans that can be used to study in vivo mechanisms of protein aggregation and that has the potential to aid the search for therapeutic modifiers of protein aggregation and toxicity.
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Affiliation(s)
- Romain F. Laine
- Laser Analytics Group, Department of Chemical Engineering and Biotechnology, University of Cambridge, Cambridge CB3 0AS, United Kingdom
| | - Tessa Sinnige
- Centre for Misfolding Diseases, Department of Chemistry, University of Cambridge, Cambridge CB2 1EW, United Kingdom
| | - Kai Yu Ma
- Centre for Misfolding Diseases, Department of Chemistry, University of Cambridge, Cambridge CB2 1EW, United Kingdom
| | - Amanda J. Haack
- Laser Analytics Group, Department of Chemical Engineering and Biotechnology, University of Cambridge, Cambridge CB3 0AS, United Kingdom
- Molecular Neuroscience Group, Department of Chemical Engineering and Biotechnology, University of Cambridge, Cambridge CB3 0AS, United Kingdom
| | - Chetan Poudel
- Laser Analytics Group, Department of Chemical Engineering and Biotechnology, University of Cambridge, Cambridge CB3 0AS, United Kingdom
| | - Peter Gaida
- Laser Analytics Group, Department of Chemical Engineering and Biotechnology, University of Cambridge, Cambridge CB3 0AS, United Kingdom
| | - Nathan Curry
- Laser Analytics Group, Department of Chemical Engineering and Biotechnology, University of Cambridge, Cambridge CB3 0AS, United Kingdom
| | - Michele Perni
- Centre for Misfolding Diseases, Department of Chemistry, University of Cambridge, Cambridge CB2 1EW, United Kingdom
| | - Ellen A.A. Nollen
- European Research Institute for the Biology of Ageing, University Medical Centre Groningen, 9700 AD Groningen, The Netherlands
| | - Christopher M. Dobson
- Centre for Misfolding Diseases, Department of Chemistry, University of Cambridge, Cambridge CB2 1EW, United Kingdom
| | - Michele Vendruscolo
- Centre for Misfolding Diseases, Department of Chemistry, University of Cambridge, Cambridge CB2 1EW, United Kingdom
| | - Gabriele S. Kaminski Schierle
- Molecular Neuroscience Group, Department of Chemical Engineering and Biotechnology, University of Cambridge, Cambridge CB3 0AS, United Kingdom
| | - Clemens F. Kaminski
- Laser Analytics Group, Department of Chemical Engineering and Biotechnology, University of Cambridge, Cambridge CB3 0AS, United Kingdom
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4
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Hochreiter B, Kunze M, Moser B, Schmid JA. Advanced FRET normalization allows quantitative analysis of protein interactions including stoichiometries and relative affinities in living cells. Sci Rep 2019; 9:8233. [PMID: 31160659 PMCID: PMC6547726 DOI: 10.1038/s41598-019-44650-0] [Citation(s) in RCA: 20] [Impact Index Per Article: 4.0] [Reference Citation Analysis] [Abstract] [Track Full Text] [Download PDF] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Received: 11/19/2018] [Accepted: 05/20/2019] [Indexed: 12/31/2022] Open
Abstract
FRET (Fluorescence Resonance Energy Transfer) measurements are commonly applied to proof protein-protein interactions. However, standard methods of live cell FRET microscopy and signal normalization only allow a principle assessment of mutual binding and are unable to deduce quantitative information of the interaction. We present an evaluation and normalization procedure for 3-filter FRET measurements, which reflects the process of complex formation by plotting FRET-saturation curves. The advantage of this approach relative to traditional signal normalizations is demonstrated by mathematical simulations. Thereby, we also identify the contribution of critical parameters such as the total amount of donor and acceptor molecules and their molar ratio. When combined with a fitting procedure, this normalization facilitates the extraction of key properties of protein complexes such as the interaction stoichiometry or the apparent affinity of the binding partners. Finally, the feasibility of our method is verified by investigating three exemplary protein complexes. Altogether, our approach offers a novel method for a quantitative analysis of protein interactions by 3-filter FRET microscopy, as well as flow cytometry. To facilitate the application of this method, we created macros and routines for the programs ImageJ, R and MS-Excel, which we make publicly available.
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Affiliation(s)
- Bernhard Hochreiter
- Medical University Vienna, Center for Physiology and Pharmacology, Institute for Vascular Biology and Thrombosis Research, Vienna, Austria
| | - Markus Kunze
- Medical University Vienna, Center for Brain Research, Department of Pathobiology of the Nervous System, Vienna, Austria
| | - Bernhard Moser
- Medical University Vienna, Center for Physiology and Pharmacology, Institute for Vascular Biology and Thrombosis Research, Vienna, Austria
| | - Johannes A Schmid
- Medical University Vienna, Center for Physiology and Pharmacology, Institute for Vascular Biology and Thrombosis Research, Vienna, Austria.
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5
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Determination of oligomerization state of Drp1 protein in living cells at nanomolar concentrations. Sci Rep 2019; 9:5906. [PMID: 30976093 PMCID: PMC6459820 DOI: 10.1038/s41598-019-42418-0] [Citation(s) in RCA: 19] [Impact Index Per Article: 3.8] [Reference Citation Analysis] [Abstract] [Track Full Text] [Download PDF] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Received: 04/19/2018] [Accepted: 03/11/2019] [Indexed: 12/15/2022] Open
Abstract
Biochemistry in living cells is an emerging field of science. Current quantitative bioassays are performed ex vivo, thus equilibrium constants and reaction rates of reactions occurring in human cells are still unknown. To address this issue, we present a non-invasive method to quantitatively characterize interactions (equilibrium constants, KD) directly within the cytosol of living cells. We reveal that cytosolic hydrodynamic drag depends exponentially on a probe's size, and provide a model for its determination for different protein sizes (1-70 nm). We analysed oligomerization of dynamin-related protein 1 (Drp1, wild type and mutants: K668E, G363D, C505A) in HeLa cells. We detected the coexistence of wt-Drp1 dimers and tetramers in cytosol, and determined that KD for tetramers was 0.7 ± 0.5 μM. Drp1 kinetics was modelled by independent simulations, giving computational results which matched experimental data. This robust method can be applied to in vivo determination of KD for other protein-protein complexes, or drug-target interactions.
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6
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Gómez CA, Sutin J, Wu W, Fu B, Uhlirova H, Devor A, Boas DA, Sakadžić S, Yaseen MA. Phasor analysis of NADH FLIM identifies pharmacological disruptions to mitochondrial metabolic processes in the rodent cerebral cortex. PLoS One 2018; 13:e0194578. [PMID: 29561904 PMCID: PMC5862490 DOI: 10.1371/journal.pone.0194578] [Citation(s) in RCA: 16] [Impact Index Per Article: 2.7] [Reference Citation Analysis] [Abstract] [MESH Headings] [Grants] [Download PDF] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Received: 09/22/2017] [Accepted: 03/06/2018] [Indexed: 01/20/2023] Open
Abstract
Investigating cerebral metabolism in vivo at a microscopic level is essential for understanding brain function and its pathological alterations. The intricate signaling and metabolic dynamics between neurons, glia, and microvasculature requires much more detailed understanding to better comprehend the mechanisms governing brain function and its disease-related changes. We recently demonstrated that pharmacologically-induced alterations to different steps of cerebral metabolism can be distinguished utilizing 2-photon fluorescence lifetime imaging of endogenous reduced nicotinamide adenine dinucleotide (NADH) fluorescence in vivo. Here, we evaluate the ability of the phasor analysis method to identify these pharmacological metabolic alterations and compare the method's performance with more conventional nonlinear curve-fitting analysis. Visualization of phasor data, both at the fundamental laser repetition frequency and its second harmonic, enables resolution of pharmacologically-induced alterations to mitochondrial metabolic processes from baseline cerebral metabolism. Compared to our previous classification models based on nonlinear curve-fitting, phasor-based models required fewer parameters and yielded comparable or improved classification accuracy. Fluorescence lifetime imaging of NADH and phasor analysis shows utility for detecting metabolic alterations and will lead to a deeper understanding of cerebral energetics and its pathological changes.
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Affiliation(s)
- Carlos A. Gómez
- Athinoula A. Martinos Center for Biomedical Imaging, Department of Radiology, Massachusetts General Hospital, Harvard Medical School, Charlestown, MA, United States of America
| | - Jason Sutin
- Athinoula A. Martinos Center for Biomedical Imaging, Department of Radiology, Massachusetts General Hospital, Harvard Medical School, Charlestown, MA, United States of America
| | - Weicheng Wu
- Athinoula A. Martinos Center for Biomedical Imaging, Department of Radiology, Massachusetts General Hospital, Harvard Medical School, Charlestown, MA, United States of America
| | - Buyin Fu
- Athinoula A. Martinos Center for Biomedical Imaging, Department of Radiology, Massachusetts General Hospital, Harvard Medical School, Charlestown, MA, United States of America
| | - Hana Uhlirova
- Department of Neurosciences and Radiology, UC San Diego, La Jolla, CA, United States of America
- Central European Institute of Technology, Brno University of Technology, Brno, Czech Republic
| | - Anna Devor
- Athinoula A. Martinos Center for Biomedical Imaging, Department of Radiology, Massachusetts General Hospital, Harvard Medical School, Charlestown, MA, United States of America
- Department of Neurosciences and Radiology, UC San Diego, La Jolla, CA, United States of America
| | - David A. Boas
- Athinoula A. Martinos Center for Biomedical Imaging, Department of Radiology, Massachusetts General Hospital, Harvard Medical School, Charlestown, MA, United States of America
| | - Sava Sakadžić
- Athinoula A. Martinos Center for Biomedical Imaging, Department of Radiology, Massachusetts General Hospital, Harvard Medical School, Charlestown, MA, United States of America
| | - Mohammad A. Yaseen
- Athinoula A. Martinos Center for Biomedical Imaging, Department of Radiology, Massachusetts General Hospital, Harvard Medical School, Charlestown, MA, United States of America
- * E-mail:
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7
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de Las Heras-Martínez G, Andrieu J, Larijani B, Requejo-Isidro J. Quantifying intracellular equilibrium dissociation constants using single-channel time-resolved FRET. JOURNAL OF BIOPHOTONICS 2018; 11:e201600272. [PMID: 28485056 DOI: 10.1002/jbio.201600272] [Citation(s) in RCA: 5] [Impact Index Per Article: 0.8] [Reference Citation Analysis] [Abstract] [Key Words] [MESH Headings] [Track Full Text] [Subscribe] [Scholar Register] [Received: 10/22/2016] [Revised: 02/20/2017] [Accepted: 02/23/2017] [Indexed: 06/07/2023]
Abstract
Quantification of the intracellular equilibrium dissociation constant of the interaction, Kd , is challenging due to the variability of the relative concentrations of the interacting proteins in the cell. Fluorescence lifetime imaging microscopy (FLIM) of the donor provides an accurate measurement of the molecular fraction of donor involved in FRET, but the fraction of bound acceptor is also needed to reliably estimate Kd . We present a method that exploits the spectroscopic properties of the widely used eGFP - mCherry FRET pair to rigorously determine the intracellular Kd based on imaging the fluorescence lifetime of only the donor (single-channel FLIM). We have assessed the effect of incomplete labelling and determined its range of application for different Kd using Monte Carlo simulations. We have demonstrated this method estimating the intracellular Kd for the homodimerisaton of the oncogenic protein 3-phosphoinositide-dependent kinase 1 (PDK1) in different cell lines and conditions, revealing a competitive mechanism for its regulation. The measured intracellular Kd was validated against in-vitro data. This method provides an accurate and generic tool to quantify protein interactions in situ.
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Affiliation(s)
| | - Josu Andrieu
- Instituto Biofisika (CSIC, UPV/EHU), Barrio de Sarriena s/n, 48940, Leioa, Spain
| | - Banafshé Larijani
- Instituto Biofisika (CSIC, UPV/EHU), Barrio de Sarriena s/n, 48940, Leioa, Spain
- Cell Biophysics Laboratory, Ikerbasque Basque Foundation for Science, Instituto Biofisika (CSIC, UPV/EHU) and Research Centre for Experimental Marine Biology and Biotechnology (PiE), University of the Basque Country (UPV/EHU), Leioa, 48940, Spain
| | - Jose Requejo-Isidro
- Instituto Biofisika (CSIC, UPV/EHU), Barrio de Sarriena s/n, 48940, Leioa, Spain
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8
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Okamoto K, Sako Y. Recent advances in FRET for the study of protein interactions and dynamics. Curr Opin Struct Biol 2017; 46:16-23. [PMID: 29800904 DOI: 10.1016/j.sbi.2017.03.010] [Citation(s) in RCA: 68] [Impact Index Per Article: 9.7] [Reference Citation Analysis] [Abstract] [MESH Headings] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Received: 12/07/2016] [Revised: 02/20/2017] [Accepted: 03/20/2017] [Indexed: 11/20/2022]
Abstract
Förster/fluorescence resonance energy transfer (FRET) has been extensively used to detect the binding state or conformation of biomolecules. In the past few decades, various in vitro and in vivo applications of FRET measurement have been developed, including FRET probes, in-cell measurements, single-molecule measurements, and combination with computer simulation. In this review, we describe recent advances in FRET methods for examining biomolecular interactions and dynamics: (i) phasor plot analysis for quantitative analysis of protein interactions, (ii) single-molecule FRET measurement for detecting conformational dynamics in live cells, and (iii) data assimilation using molecular dynamics simulation to evaluate conformation of the whole protein.
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Affiliation(s)
- Kenji Okamoto
- Cellular Informatics Laboratory, RIKEN, 2-1 Hirosawa, Wako, Saitama 351-0198, Japan.
| | - Yasushi Sako
- Cellular Informatics Laboratory, RIKEN, 2-1 Hirosawa, Wako, Saitama 351-0198, Japan
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9
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Blacker T, Chen W, Avezov E, Marsh RJ, Duchen MR, Kaminski CF, Bain AJ. Investigating State Restriction in Fluorescent Protein FRET Using Time-Resolved Fluorescence and Anisotropy. THE JOURNAL OF PHYSICAL CHEMISTRY. C, NANOMATERIALS AND INTERFACES 2017; 121:1507-1514. [PMID: 28217242 PMCID: PMC5309863 DOI: 10.1021/acs.jpcc.6b11235] [Citation(s) in RCA: 7] [Impact Index Per Article: 1.0] [Reference Citation Analysis] [Abstract] [Grants] [Track Full Text] [Subscribe] [Scholar Register] [Received: 11/08/2016] [Revised: 12/23/2016] [Indexed: 05/14/2023]
Abstract
Most fluorescent proteins exhibit multiexponential fluorescence decays, indicating a heterogeneous excited state population. FRET between fluorescent proteins should therefore involve multiple energy transfer pathways. We recently demonstrated the FRET pathways between EGFP and mCherry (mC), upon the dimerization of 3-phosphoinositide dependent protein kinase 1 (PDK1), to be highly restricted. A mechanism for FRET restriction based on a highly unfavorable κ2 orientation factor arising from differences in donor-acceptor transition dipole moment angles in a far from coplanar and near static interaction geometry was proposed. Here this is tested via FRET to mC arising from the association of glutathione (GSH) and glutathione S-transferase (GST) with an intrinsically homogeneous and more mobile donor Oregon Green 488 (OG). A new analysis of the acceptor window intensity, based on the turnover point of the sensitized fluorescence, is combined with donor window intensity and anisotropy measurements which show that unrestricted FRET to mC takes place. However, a long-lived anisotropy decay component in the donor window reveals a GST-GSH population in which FRET does not occur, explaining previous discrepancies between quantitative FRET measurements of GST-GSH association and their accepted values. This reinforces the importance of the local donor-acceptor environment in mediating energy transfer and the need to perform spectrally resolved intensity and anisotropy decay measurements in the accurate quantification of fluorescent protein FRET.
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Affiliation(s)
- Thomas
S. Blacker
- Department
of Physics & Astronomy, Centre for Mathematics and Physics
in the Life Sciences and Experimental Biology, and Department of Cell & Developmental
Biology, University College London, Gower Street, London WC1E 6BT, United
Kingdom
| | - WeiYue Chen
- Department
of Chemical Engineering and Biotechnology, University of Cambridge, Pembroke Street, Cambridge CB2 3RA, United Kingdom
| | - Edward Avezov
- Cambridge
Institute for Medical Research, University
of Cambridge, Cambridge CB2 0XY, United Kingdom
| | - Richard J. Marsh
- Department
of Physics & Astronomy, Centre for Mathematics and Physics
in the Life Sciences and Experimental Biology, and Department of Cell & Developmental
Biology, University College London, Gower Street, London WC1E 6BT, United
Kingdom
| | - Michael R. Duchen
- Department
of Physics & Astronomy, Centre for Mathematics and Physics
in the Life Sciences and Experimental Biology, and Department of Cell & Developmental
Biology, University College London, Gower Street, London WC1E 6BT, United
Kingdom
| | - Clemens F. Kaminski
- Department
of Chemical Engineering and Biotechnology, University of Cambridge, Pembroke Street, Cambridge CB2 3RA, United Kingdom
| | - Angus J. Bain
- Department
of Physics & Astronomy, Centre for Mathematics and Physics
in the Life Sciences and Experimental Biology, and Department of Cell & Developmental
Biology, University College London, Gower Street, London WC1E 6BT, United
Kingdom
- E-mail:
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10
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Chen W, Young LJ, Lu M, Zaccone A, Ströhl F, Yu N, Kaminski Schierle GS, Kaminski CF. Fluorescence Self-Quenching from Reporter Dyes Informs on the Structural Properties of Amyloid Clusters Formed in Vitro and in Cells. NANO LETTERS 2017; 17:143-149. [PMID: 28073262 PMCID: PMC5338000 DOI: 10.1021/acs.nanolett.6b03686] [Citation(s) in RCA: 37] [Impact Index Per Article: 5.3] [Reference Citation Analysis] [Abstract] [Key Words] [MESH Headings] [Grants] [Track Full Text] [Subscribe] [Scholar Register] [Received: 09/01/2016] [Revised: 10/26/2016] [Indexed: 05/26/2023]
Abstract
The characterization of the aggregation kinetics of protein amyloids and the structural properties of the ensuing aggregates are vital in the study of the pathogenesis of many neurodegenerative diseases and the discovery of therapeutic targets. In this article, we show that the fluorescence lifetime of synthetic dyes covalently attached to amyloid proteins informs on the structural properties of amyloid clusters formed both in vitro and in cells. We demonstrate that the mechanism behind such a "lifetime sensor" of protein aggregation is based on fluorescence self-quenching and that it offers a good dynamic range to report on various stages of aggregation without significantly perturbing the process under investigation. We show that the sensor informs on the structural density of amyloid clusters in a high-throughput and quantitative manner and in these aspects the sensor outperforms super-resolution imaging techniques. We demonstrate the power and speed of the method, offering capabilities, for example, in therapeutic screenings that monitor biological self-assembly. We investigate the mechanism and advantages of the lifetime sensor in studies of the K18 protein fragment of the Alzheimer's disease related protein tau and its amyloid aggregates formed in vitro. Finally, we demonstrate the sensor in the study of aggregates of polyglutamine protein, a model used in studies related to Huntington's disease, by performing correlative fluorescence lifetime imaging microscopy and structured-illumination microscopy experiments in cells.
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11
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Kaye B, Foster PJ, Yoo TY, Needleman DJ. Developing and Testing a Bayesian Analysis of Fluorescence Lifetime Measurements. PLoS One 2017; 12:e0169337. [PMID: 28060890 PMCID: PMC5217968 DOI: 10.1371/journal.pone.0169337] [Citation(s) in RCA: 20] [Impact Index Per Article: 2.9] [Reference Citation Analysis] [Abstract] [MESH Headings] [Grants] [Track Full Text] [Download PDF] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Received: 07/12/2016] [Accepted: 12/15/2016] [Indexed: 11/18/2022] Open
Abstract
FRET measurements can provide dynamic spatial information on length scales smaller than the diffraction limit of light. Several methods exist to measure FRET between fluorophores, including Fluorescence Lifetime Imaging Microscopy (FLIM), which relies on the reduction of fluorescence lifetime when a fluorophore is undergoing FRET. FLIM measurements take the form of histograms of photon arrival times, containing contributions from a mixed population of fluorophores both undergoing and not undergoing FRET, with the measured distribution being a mixture of exponentials of different lifetimes. Here, we present an analysis method based on Bayesian inference that rigorously takes into account several experimental complications. We test the precision and accuracy of our analysis on controlled experimental data and verify that we can faithfully extract model parameters, both in the low-photon and low-fraction regimes.
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Affiliation(s)
- Bryan Kaye
- John A. Paulson School of Engineering and Applied Sciences, Harvard University, Cambridge, MA, United States of America
- FAS Center for Systems Biology, Harvard University, Cambridge, MA, United States of America
- * E-mail:
| | - Peter J. Foster
- John A. Paulson School of Engineering and Applied Sciences, Harvard University, Cambridge, MA, United States of America
- FAS Center for Systems Biology, Harvard University, Cambridge, MA, United States of America
| | - Tae Yeon Yoo
- John A. Paulson School of Engineering and Applied Sciences, Harvard University, Cambridge, MA, United States of America
- FAS Center for Systems Biology, Harvard University, Cambridge, MA, United States of America
| | - Daniel J. Needleman
- John A. Paulson School of Engineering and Applied Sciences, Harvard University, Cambridge, MA, United States of America
- FAS Center for Systems Biology, Harvard University, Cambridge, MA, United States of America
- Department of Molecular and Cellular Biology, Harvard University, Cambridge, MA, United States of America
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12
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Gielen F, Butz M, Rees EJ, Erdelyi M, Moschetti T, Hyvönen M, Edel JB, Kaminski CF, Hollfelder F. Quantitative Affinity Determination by Fluorescence Anisotropy Measurements of Individual Nanoliter Droplets. Anal Chem 2017; 89:1092-1101. [PMID: 28192993 PMCID: PMC5287478 DOI: 10.1021/acs.analchem.6b02528] [Citation(s) in RCA: 24] [Impact Index Per Article: 3.4] [Reference Citation Analysis] [Abstract] [Track Full Text] [Download PDF] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Indexed: 01/23/2023]
Abstract
Fluorescence anisotropy measurements of reagents compartmentalized into individual nanoliter droplets are shown to yield high-resolution binding curves from which precise dissociation constants (Kd) for protein-peptide interactions can be inferred. With the current platform, four titrations can be obtained per minute (based on ∼100 data points each), with stoichiometries spanning more than 2 orders of magnitude and requiring only tens of microliters of reagents. In addition to affinity measurements with purified components, Kd values for unpurified proteins in crude cell lysates can be obtained without prior knowledge of the concentration of the expressed protein, so that protein purification can be avoided. Finally, we show how a competition assay can be set up to perform focused library screens, so that compound labeling is not required anymore. These data demonstrate the utility of droplet compartments for the quantitative characterization of biomolecular interactions and establish fluorescence anisotropy imaging as a quantitative technique in a miniaturized droplet format, which is shown to be as reliable as its macroscopic test tube equivalent.
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Affiliation(s)
- Fabrice Gielen
- Department of Biochemistry, University of Cambridge , 80 Tennis Court Road, Cambridge, CB2 1GA, United Kingdom.,Living Systems Institute, University of Exeter , Stocker Road, Exeter, EX4 4QD, United Kingdom
| | - Maren Butz
- Department of Biochemistry, University of Cambridge , 80 Tennis Court Road, Cambridge, CB2 1GA, United Kingdom
| | - Eric J Rees
- Department of Chemical Engineering and Biotechnology, New Museums Site , Pembroke Street, Cambridge, CB2 3RA, United Kingdom
| | - Miklos Erdelyi
- Department of Chemical Engineering and Biotechnology, New Museums Site , Pembroke Street, Cambridge, CB2 3RA, United Kingdom.,Department of Optics and Quantum Electronics, University of Szeged , Dom ter 9, Szeged, Hungary
| | - Tommaso Moschetti
- Department of Biochemistry, University of Cambridge , 80 Tennis Court Road, Cambridge, CB2 1GA, United Kingdom
| | - Marko Hyvönen
- Department of Biochemistry, University of Cambridge , 80 Tennis Court Road, Cambridge, CB2 1GA, United Kingdom
| | - Joshua B Edel
- Department of Chemistry, Imperial College London , South Kensington, London, SW7 2AZ, United Kingdom
| | - Clemens F Kaminski
- Department of Chemical Engineering and Biotechnology, New Museums Site , Pembroke Street, Cambridge, CB2 3RA, United Kingdom
| | - Florian Hollfelder
- Department of Biochemistry, University of Cambridge , 80 Tennis Court Road, Cambridge, CB2 1GA, United Kingdom
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13
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Losada A, Muñoz-Alonso MJ, García C, Sánchez-Murcia PA, Martínez-Leal JF, Domínguez JM, Lillo MP, Gago F, Galmarini CM. Translation Elongation Factor eEF1A2 is a Novel Anticancer Target for the Marine Natural Product Plitidepsin. Sci Rep 2016; 6:35100. [PMID: 27713531 PMCID: PMC5054363 DOI: 10.1038/srep35100] [Citation(s) in RCA: 63] [Impact Index Per Article: 7.9] [Reference Citation Analysis] [Abstract] [Track Full Text] [Download PDF] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Received: 04/15/2016] [Accepted: 09/22/2016] [Indexed: 12/18/2022] Open
Abstract
eEF1A2 is one of the isoforms of the alpha subunit of the eukaryotic Elongation Factor 1. It is overexpressed in human tumors and is endowed with oncogenic properties, favoring tumor cell proliferation while inhibiting apoptosis. We demonstrate that plitidepsin, an antitumor agent of marine origin that has successfully completed a phase-III clinical trial for multiple myeloma, exerts its antitumor activity by targeting eEF1A2. The drug interacts with eEF1A2 with a KD of 80 nM and a target residence time of circa 9 min. This protein was also identified as capable of binding [14C]-plitidepsin in a cell lysate from K-562 tumor cells. A molecular modelling approach was used to identify a favorable binding site for plitidepsin at the interface between domains 1 and 2 of eEF1A2 in the GTP conformation. Three tumor cell lines selected for at least 100-fold more resistance to plitidepsin than their respective parental cells showed reduced levels of eEF1A2 protein. Ectopic expression of eEF1A2 in resistant cells restored the sensitivity to plitidepsin. FLIM-phasor FRET experiments demonstrated that plitidepsin localizes in tumor cells sufficiently close to eEF1A2 as to suggest the formation of drug-protein complexes in living cells. Altogether, our results strongly suggest that eEF1A2 is the primary target of plitidepsin.
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Affiliation(s)
- Alejandro Losada
- Departamento de Biología Celular y Farmacogenómica, Pharma Mar S.A., Colmenar Viejo, Madrid, Spain
| | - María José Muñoz-Alonso
- Departamento de Biología Celular y Farmacogenómica, Pharma Mar S.A., Colmenar Viejo, Madrid, Spain
| | - Carolina García
- Departamento de Química Física Biológica, Instituto de Química-Física "Rocasolano" (CSIC), Madrid, Spain
| | - Pedro A Sánchez-Murcia
- Departamento de Ciencias Biomédicas, Unidad Asociada al IQM-CSIC, Universidad de Alcalá, Madrid, Spain
| | | | - Juan Manuel Domínguez
- Departamento de Biología Celular y Farmacogenómica, Pharma Mar S.A., Colmenar Viejo, Madrid, Spain
| | - M Pilar Lillo
- Departamento de Química Física Biológica, Instituto de Química-Física "Rocasolano" (CSIC), Madrid, Spain
| | - Federico Gago
- Departamento de Ciencias Biomédicas, Unidad Asociada al IQM-CSIC, Universidad de Alcalá, Madrid, Spain
| | - Carlos M Galmarini
- Departamento de Biología Celular y Farmacogenómica, Pharma Mar S.A., Colmenar Viejo, Madrid, Spain
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14
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Buntru A, Trepte P, Klockmeier K, Schnoegl S, Wanker EE. Current Approaches Toward Quantitative Mapping of the Interactome. Front Genet 2016; 7:74. [PMID: 27200083 PMCID: PMC4854875 DOI: 10.3389/fgene.2016.00074] [Citation(s) in RCA: 18] [Impact Index Per Article: 2.3] [Reference Citation Analysis] [Abstract] [Key Words] [Track Full Text] [Download PDF] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Received: 12/23/2015] [Accepted: 04/18/2016] [Indexed: 01/01/2023] Open
Abstract
Protein–protein interactions (PPIs) play a key role in many, if not all, cellular processes. Disease is often caused by perturbation of PPIs, as recently indicated by studies of missense mutations. To understand the associations of proteins and to unravel the global picture of PPIs in the cell, different experimental detection techniques for PPIs have been established. Genetic and biochemical methods such as the yeast two-hybrid system or affinity purification-based approaches are well suited to high-throughput, proteome-wide screening and are mainly used to obtain qualitative results. However, they have been criticized for not reflecting the cellular situation or the dynamic nature of PPIs. In this review, we provide an overview of various genetic methods that go beyond qualitative detection and allow quantitative measuring of PPIs in mammalian cells, such as dual luminescence-based co-immunoprecipitation, Förster resonance energy transfer or luminescence-based mammalian interactome mapping with bait control. We discuss the strengths and weaknesses of different techniques and their potential applications in biomedical research.
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Affiliation(s)
| | - Philipp Trepte
- Max Delbrueck Center for Molecular Medicine Berlin, Germany
| | | | | | - Erich E Wanker
- Max Delbrueck Center for Molecular Medicine Berlin, Germany
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15
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Popleteeva M, Haas KT, Stoppa D, Pancheri L, Gasparini L, Kaminski CF, Cassidy LD, Venkitaraman AR, Esposito A. Fast and simple spectral FLIM for biochemical and medical imaging. OPTICS EXPRESS 2015; 23:23511-25. [PMID: 26368450 DOI: 10.1364/oe.23.023511] [Citation(s) in RCA: 14] [Impact Index Per Article: 1.6] [Reference Citation Analysis] [Abstract] [MESH Headings] [Grants] [Track Full Text] [Subscribe] [Scholar Register] [Indexed: 05/23/2023]
Abstract
Spectrally resolved fluorescence lifetime imaging microscopy (λFLIM) has powerful potential for biochemical and medical imaging applications. However, long acquisition times, low spectral resolution and complexity of λFLIM often narrow its use to specialized laboratories. Therefore, we demonstrate here a simple spectral FLIM based on a solid-state detector array providing in-pixel histrogramming and delivering faster acquisition, larger dynamic range, and higher spectral elements than state-of-the-art λFLIM. We successfully apply this novel microscopy system to biochemical and medical imaging demonstrating that solid-state detectors are a key strategic technology to enable complex assays in biomedical laboratories and the clinic.
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