1
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Hughes JW, Sisley EK, Hale OJ, Cooper HJ. Laser capture microdissection and native mass spectrometry for spatially-resolved analysis of intact protein assemblies in tissue. Chem Sci 2024; 15:5723-5729. [PMID: 38638209 PMCID: PMC11023061 DOI: 10.1039/d3sc04933g] [Citation(s) in RCA: 0] [Impact Index Per Article: 0] [Reference Citation Analysis] [Abstract] [Grants] [Track Full Text] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Received: 09/19/2023] [Accepted: 03/03/2024] [Indexed: 04/20/2024] Open
Abstract
Previously, we have shown that native ambient mass spectrometry imaging allows the spatial mapping of folded proteins and their complexes in thin tissue sections. Subsequent top-down native ambient mass spectrometry of adjacent tissue section enables protein identification. The challenges associated with protein identification by this approach are (i) the low abundance of proteins in tissue and associated long data acquisition timescales and (ii) irregular spatial distributions which hamper targeted sampling of the relevant tissue location. Here, we demonstrate that these challenges may be overcome through integration of laser capture microdissection in the workflow. We show identification of intact protein assemblies in rat liver tissue and apply the approach to identification of proteins in the granular layer of rat cerebellum.
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Affiliation(s)
- James W Hughes
- School of Biosciences, University of Birmingham Edgbaston Birmingham B15 2TT UK
| | - Emma K Sisley
- School of Biosciences, University of Birmingham Edgbaston Birmingham B15 2TT UK
| | - Oliver J Hale
- School of Biosciences, University of Birmingham Edgbaston Birmingham B15 2TT UK
| | - Helen J Cooper
- School of Biosciences, University of Birmingham Edgbaston Birmingham B15 2TT UK
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2
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Suvannapruk W, Fisher LE, Luckett JC, Edney MK, Kotowska AM, Kim D, Scurr DJ, Ghaemmaghami AM, Alexander MR. Spatially Resolved Molecular Analysis of Host Response to Medical Device Implantation Using the 3D OrbiSIMS Highlights a Critical Role for Lipids. ADVANCED SCIENCE (WEINHEIM, BADEN-WURTTEMBERG, GERMANY) 2024; 11:e2306000. [PMID: 38356246 PMCID: PMC11022720 DOI: 10.1002/advs.202306000] [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: 08/23/2023] [Revised: 01/18/2024] [Indexed: 02/16/2024]
Abstract
A key goal for implanted medical devices is that they do not elicit a detrimental immune response. Macrophages play critical roles in the modulation of the host immune response and are the cells responsible for persistent inflammatory reactions to implanted biomaterials. Two novel immune-instructive polymers that stimulate pro- or anti-inflammatory responses from macrophages in vitro are investigated. These also modulate in vivo foreign body responses (FBR) when implanted subcutaneously in mice. Immunofluorescent staining of tissue abutting the polymer reveals responses consistent with pro- or anti-inflammatory responses previously described for these polymers. Three Dimensional OrbiTrap Secondary Ion Mass Spectrometry (3D OrbiSIMS) analysis to spatially characterize the metabolites in the tissue surrounding the implant, providing molecular histology insight into the metabolite response in the host is applied. For the pro-inflammatory polymer, monoacylglycerols (MG) and diacylglycerols (DG) are observed at increased intensity, while for the anti-inflammatory coating, the number of phospholipid species detected decreased, and pyridine and pyrimidine levels are elevated. Small molecule signatures from single-cell studies of M2 macrophages in vitro correlate with the in vivo observations, suggesting potential for prediction. Metabolite characterization by the 3D OrbiSIMS is shown to provide insight into the mechanism of bio-instructive materials as medical devices and to inform on the FBR to biomaterials.
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Affiliation(s)
- Waraporn Suvannapruk
- Advanced Materials and Healthcare Technologies DivisionSchool of PharmacyUniversity of NottinghamUniversity Park NottinghamNottinghamNG7 2RDUK
- Present address:
National Metal and Materials Technology Center (MTEC)114 Thailand Science Park, Phahonyothin Road, Khlong Nueng, Khlong LuangPathum Thani12120Thailand
| | - Leanne E Fisher
- Advanced Materials and Healthcare Technologies DivisionSchool of PharmacyUniversity of NottinghamUniversity Park NottinghamNottinghamNG7 2RDUK
| | - Jeni C Luckett
- School of Life SciencesFaculty of Medicine and Health ScienceUniversity of NottinghamUniversity Park NottinghamNottinghamNG7 2RDUK
| | - Max K Edney
- Department of Chemical and Environmental EngineeringFaculty of EngineeringUniversity of NottinghamUniversity Park NottinghamNottinghamNG7 2RDUK
| | - Anna M Kotowska
- Advanced Materials and Healthcare Technologies DivisionSchool of PharmacyUniversity of NottinghamUniversity Park NottinghamNottinghamNG7 2RDUK
| | - Dong‐Hyun Kim
- Advanced Materials and Healthcare Technologies DivisionSchool of PharmacyUniversity of NottinghamUniversity Park NottinghamNottinghamNG7 2RDUK
| | - David J Scurr
- Advanced Materials and Healthcare Technologies DivisionSchool of PharmacyUniversity of NottinghamUniversity Park NottinghamNottinghamNG7 2RDUK
| | - Amir M Ghaemmaghami
- Immunology & Immuno‐bioengineering GroupSchool of Life SciencesFaculty of Medicine and Health SciencesUniversity of NottinghamUniversity Park NottinghamNottinghamNG7 2RDUK
| | - Morgan R Alexander
- Advanced Materials and Healthcare Technologies DivisionSchool of PharmacyUniversity of NottinghamUniversity Park NottinghamNottinghamNG7 2RDUK
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3
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Yan M, Zhang N, Li X, Xu J, Lei H, Ma Q. Integrating Post-Ionization Separation via Differential Mobility Spectrometry into Direct Analysis in Real Time Mass Spectrometry for Toy Safety Screening. Anal Chem 2024; 96:265-271. [PMID: 38153235 DOI: 10.1021/acs.analchem.3c03915] [Citation(s) in RCA: 0] [Impact Index Per Article: 0] [Reference Citation Analysis] [Abstract] [MESH Headings] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Indexed: 12/29/2023]
Abstract
Direct analysis in real time (DART) enables direct desorption and ionization of analytes, bypassing the time-consuming chromatographic separation traditionally required for mass spectrometry (MS) analysis. However, DART-MS suffers from matrix interference of complex samples, resulting in compromised detection sensitivity and quantitation accuracy. In this study, DART-MS was combined with differential mobility spectrometry (DMS) to provide an additional dimension of post-ionization ion mobility separation within a millisecond time scale, compensating for the lack of separation in DART-MS analysis. As proof-of-concept, primary aromatic amines (PAAs), a class of potentially hazardous chemicals, were analyzed in various toy products, including bubble solutions, finger paints, and plush toys. In addition to commercial Dip-it glass rod and metal mesh sampling tools, a customized rapid extractive evaporation device was designed for the accelerated extraction and sensitive analysis of solid toy samples. The incorporation of DMS in DART-MS analysis enabled the rapid separation and differentiation of isomeric analytes, leading to improved accuracy and reliability. The developed protocols were optimized and validated, achieving good linearity with correlation coefficients greater than 0.99 and acceptable repeatability with relative standard deviations less than 10%. Moreover, satisfactory sensitivity was realized with limits of detection and quantitation ranges of 0.2-5 and 1-20 μg/kg (μg/L) for the 11 PAA analytes. The established methodology was applied for the analysis of real toy samples (n = 18), which confirmed its appealing potential for toy safety screening and consumer health protection.
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Affiliation(s)
- Mengmeng Yan
- Key Laboratory of Consumer Product Quality Safety Inspection and Risk Assessment for State Market Regulation, Chinese Academy of Inspection and Quarantine, Beijing 100176, China
- Beijing Anti-Doping Laboratory, Beijing Sport University, Beijing 100091, China
| | - Nan Zhang
- Key Laboratory of Consumer Product Quality Safety Inspection and Risk Assessment for State Market Regulation, Chinese Academy of Inspection and Quarantine, Beijing 100176, China
- School of Life and Pharmaceutical Sciences, Dalian University of Technology, Panjin 124221, China
| | - Xiaoxu Li
- School of Mechanical and Electrical Engineering, Soochow University, Suzhou 215021, China
| | - Jianqiang Xu
- School of Life and Pharmaceutical Sciences, Dalian University of Technology, Panjin 124221, China
| | - Haimin Lei
- School of Chinese Materia Medica, Beijing University of Chinese Medicine, Beijing 102488, China
| | - Qiang Ma
- Key Laboratory of Consumer Product Quality Safety Inspection and Risk Assessment for State Market Regulation, Chinese Academy of Inspection and Quarantine, Beijing 100176, China
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4
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Nickerson JL, Baghalabadi V, Rajendran SRCK, Jakubec PJ, Said H, McMillen TS, Dang Z, Doucette AA. Recent advances in top-down proteome sample processing ahead of MS analysis. MASS SPECTROMETRY REVIEWS 2023; 42:457-495. [PMID: 34047392 DOI: 10.1002/mas.21706] [Citation(s) in RCA: 18] [Impact Index Per Article: 18.0] [Reference Citation Analysis] [Abstract] [Key Words] [MESH Headings] [Track Full Text] [Subscribe] [Scholar Register] [Received: 02/19/2021] [Revised: 04/21/2021] [Accepted: 05/06/2021] [Indexed: 06/12/2023]
Abstract
Top-down proteomics is emerging as a preferred approach to investigate biological systems, with objectives ranging from the detailed assessment of a single protein therapeutic, to the complete characterization of every possible protein including their modifications, which define the human proteoform. Given the controlling influence of protein modifications on their biological function, understanding how gene products manifest or respond to disease is most precisely achieved by characterization at the intact protein level. Top-down mass spectrometry (MS) analysis of proteins entails unique challenges associated with processing whole proteins while maintaining their integrity throughout the processes of extraction, enrichment, purification, and fractionation. Recent advances in each of these critical front-end preparation processes, including minimalistic workflows, have greatly expanded the capacity of MS for top-down proteome analysis. Acknowledging the many contributions in MS technology and sample processing, the present review aims to highlight the diverse strategies that have forged a pathway for top-down proteomics. We comprehensively discuss the evolution of front-end workflows that today facilitate optimal characterization of proteoform-driven biology, including a brief description of the clinical applications that have motivated these impactful contributions.
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Affiliation(s)
| | - Venus Baghalabadi
- Department of Chemistry, Dalhousie University, Halifax, Nova Scotia, Canada
| | - Subin R C K Rajendran
- Department of Chemistry, Dalhousie University, Halifax, Nova Scotia, Canada
- Verschuren Centre for Sustainability in Energy and the Environment, Sydney, Nova Scotia, Canada
| | - Philip J Jakubec
- Department of Chemistry, Dalhousie University, Halifax, Nova Scotia, Canada
| | - Hammam Said
- Department of Chemistry, Dalhousie University, Halifax, Nova Scotia, Canada
| | - Teresa S McMillen
- Department of Chemistry, Dalhousie University, Halifax, Nova Scotia, Canada
| | - Ziheng Dang
- Department of Chemistry, Dalhousie University, Halifax, Nova Scotia, Canada
| | - Alan A Doucette
- Department of Chemistry, Dalhousie University, Halifax, Nova Scotia, Canada
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5
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Surface-sampling mass spectrometry to study proteins and protein complexes. Essays Biochem 2023; 67:229-241. [PMID: 36748325 PMCID: PMC10070487 DOI: 10.1042/ebc20220191] [Citation(s) in RCA: 5] [Impact Index Per Article: 5.0] [Reference Citation Analysis] [Abstract] [Key Words] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Received: 10/11/2022] [Revised: 01/03/2023] [Accepted: 01/05/2023] [Indexed: 02/08/2023]
Abstract
This review aims to summarise the current capabilities of surface mass spectrometry (MS) approaches that offer intact protein analysis, and that of non-covalent complexes. Protein analysis is largely achieved via matrix-assisted laser desorption/ionisation (MALDI), which is in itself a surface analysis approach or solvent-based electrospray ionisation (ESI). Several surface sampling approaches have been developed based on ESI, and those that have been used for intact protein analysis will be discussed below. The extent of protein coverage, top-down elucidation, and probing of protein structure for native proteins and non-covalent complexes will be discussed for each approach. Strategies for improving protein analysis, ranging from sample preparation, and sampling methods to instrument modifications and the inclusion of ion mobility separation in the workflow will also be discussed. The relative benefits and drawbacks of each approach will be summarised, providing an overview of current capabilities.
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6
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Hou JJ, Zhang ZJ, Wu WY, He QQ, Zhang TQ, Liu YW, Wang ZJ, Gao L, Long HL, Lei M, Wu WY, Guo DA. Mass spectrometry imaging: new eyes on natural products for drug research and development. Acta Pharmacol Sin 2022; 43:3096-3111. [PMID: 36229602 PMCID: PMC9712638 DOI: 10.1038/s41401-022-00990-8] [Citation(s) in RCA: 7] [Impact Index Per Article: 3.5] [Reference Citation Analysis] [Abstract] [Key Words] [MESH Headings] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Received: 06/13/2022] [Accepted: 08/25/2022] [Indexed: 11/09/2022] Open
Abstract
Natural products (NPs) and their structural analogs represent a major source of novel drug development for disease prevention and treatment. The development of new drugs from NPs includes two crucial aspects. One is the discovery of NPs from medicinal plants/microorganisms, and the other is the evaluation of the NPs in vivo at various physiological and pathological states. The heterogeneous spatial distribution of NPs in medicinal plants/microorganisms or in vivo can provide valuable information for drug development. However, few molecular imaging technologies can detect thousands of compounds simultaneously on a label-free basis. Over the last two decades, mass spectrometry imaging (MSI) methods have progressively improved and diversified, thereby allowing for the development of various applications of NPs in plants/microorganisms and in vivo NP research. Because MSI allows for the spatial mapping of the production and distribution of numerous molecules in situ without labeling, it provides a visualization tool for NP research. Therefore, we have focused this mini-review on summarizing the applications of MSI technology in discovering NPs from medicinal plants and evaluating NPs in preclinical studies from the perspective of new drug research and development (R&D). Additionally, we briefly reviewed the factors that should be carefully considered to obtain the desired MSI results. Finally, the future development of MSI in new drug R&D is proposed.
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Affiliation(s)
- Jin-Jun Hou
- National Engineering Research Center of TCM Standardization Technology, Shanghai Institute of Materia Medica, Chinese Academy of Sciences, Shanghai, 201203, China
- University of Chinese Academy of Sciences, Beijing, 100049, China
| | - Zi-Jia Zhang
- National Engineering Research Center of TCM Standardization Technology, Shanghai Institute of Materia Medica, Chinese Academy of Sciences, Shanghai, 201203, China
- University of Chinese Academy of Sciences, Beijing, 100049, China
| | - Wen-Yong Wu
- National Engineering Research Center of TCM Standardization Technology, Shanghai Institute of Materia Medica, Chinese Academy of Sciences, Shanghai, 201203, China
- School of Chinese Materia Medica, Nanjing University of Chinese Medicine, Nanjing, 210029, China
| | - Qing-Qing He
- National Engineering Research Center of TCM Standardization Technology, Shanghai Institute of Materia Medica, Chinese Academy of Sciences, Shanghai, 201203, China
| | - Teng-Qian Zhang
- National Engineering Research Center of TCM Standardization Technology, Shanghai Institute of Materia Medica, Chinese Academy of Sciences, Shanghai, 201203, China
- University of Chinese Academy of Sciences, Beijing, 100049, China
| | - Ya-Wen Liu
- National Engineering Research Center of TCM Standardization Technology, Shanghai Institute of Materia Medica, Chinese Academy of Sciences, Shanghai, 201203, China
- University of Chinese Academy of Sciences, Beijing, 100049, China
| | - Zhao-Jun Wang
- National Engineering Research Center of TCM Standardization Technology, Shanghai Institute of Materia Medica, Chinese Academy of Sciences, Shanghai, 201203, China
- University of Chinese Academy of Sciences, Beijing, 100049, China
| | - Lei Gao
- National Engineering Research Center of TCM Standardization Technology, Shanghai Institute of Materia Medica, Chinese Academy of Sciences, Shanghai, 201203, China
- University of Chinese Academy of Sciences, Beijing, 100049, China
| | - Hua-Li Long
- National Engineering Research Center of TCM Standardization Technology, Shanghai Institute of Materia Medica, Chinese Academy of Sciences, Shanghai, 201203, China
- University of Chinese Academy of Sciences, Beijing, 100049, China
| | - Min Lei
- National Engineering Research Center of TCM Standardization Technology, Shanghai Institute of Materia Medica, Chinese Academy of Sciences, Shanghai, 201203, China
- University of Chinese Academy of Sciences, Beijing, 100049, China
| | - Wan-Ying Wu
- National Engineering Research Center of TCM Standardization Technology, Shanghai Institute of Materia Medica, Chinese Academy of Sciences, Shanghai, 201203, China.
- University of Chinese Academy of Sciences, Beijing, 100049, China.
| | - De-An Guo
- National Engineering Research Center of TCM Standardization Technology, Shanghai Institute of Materia Medica, Chinese Academy of Sciences, Shanghai, 201203, China.
- University of Chinese Academy of Sciences, Beijing, 100049, China.
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7
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Rickert D, Gómez-Ríos GA, Singh V, Pawliszyn J. Understanding the effect of spatial positioning of coated blade spray devices relative to the mass spectrometry inlet on different instrument platforms and its application to quantitative analysis of fentanyl and related analogs. RAPID COMMUNICATIONS IN MASS SPECTROMETRY : RCM 2022; 36:e9388. [PMID: 36039809 DOI: 10.1002/rcm.9388] [Citation(s) in RCA: 2] [Impact Index Per Article: 1.0] [Reference Citation Analysis] [Abstract] [MESH Headings] [Track Full Text] [Subscribe] [Scholar Register] [Received: 06/20/2022] [Revised: 08/29/2022] [Accepted: 08/29/2022] [Indexed: 06/15/2023]
Abstract
RATIONALE We evaluated the effect that the spatial positioning of coated-blade spray (CBS) devices with respect to the mass spectrometry (MS) inlet has when coupling to diverse MS platforms (i.e., triple quadrupole, linear ion trap and time of flight). Furthermore, as a proof of concept, we evaluated CBS-MS as a tool for quantitation of fentanyl and four analogues on said instruments. METHODS Custom-made MS interfaces were made to accurately position the blade in front of the MS inlet. CBS devices, coated with hydrophilic-lipophilic balanced particles, were used for both the optimization of the CBS position and the quantitation of fentanyl and analogues in urine and plasma samples on all instruments. RESULTS The SCIEX triple quadrupole instrument was the most sensitive to the position of the blade due to the presence of a curtain gas flowing laminarly out of the MS inlet. After optimization, the analytical capabilities of CBS on each instrument were assessed and the results obtained on both SCIEX and Waters platforms matched the performance obtained using a more advanced instrument by ThermoFisher Scientific. Furthermore, excellent figures of merit were attained for the quantitation of fentanyl and analogues on both triple quadrupole and linear ion trap platforms. CONCLUSIONS We demonstrated that optimization of MS parameters on different instrument vendors and front ends, such as the position of the CBS tip regarding the MS inlet, is vital to exploit the full quantitative potential of this technology. Application of the technology to screen and quantify fentanyl and analogues showed great potential when considering its coupling with portable mass spectrometers for therapeutic drug monitoring and point-of-care applications.
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Affiliation(s)
- Daniel Rickert
- Department of Chemistry, University of Waterloo, Waterloo, ON, Canada
| | | | - Varoon Singh
- Department of Chemistry, University of Waterloo, Waterloo, ON, Canada
| | - Janusz Pawliszyn
- Department of Chemistry, University of Waterloo, Waterloo, ON, Canada
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8
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Li L, Sun C, Sun Y, Dong Z, Wu R, Sun X, Zhang H, Jiang W, Zhou Y, Cen X, Cai S, Xia H, Zhu Y, Guo T, Piatkevich KD. Spatially resolved proteomics via tissue expansion. Nat Commun 2022; 13:7242. [PMID: 36450705 PMCID: PMC9712279 DOI: 10.1038/s41467-022-34824-2] [Citation(s) in RCA: 11] [Impact Index Per Article: 5.5] [Reference Citation Analysis] [Abstract] [Key Words] [Track Full Text] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Received: 01/13/2022] [Accepted: 11/04/2022] [Indexed: 12/12/2022] Open
Abstract
Spatially resolved proteomics is an emerging approach for mapping proteome heterogeneity of biological samples, however, it remains technically challenging due to the complexity of the tissue microsampling techniques and mass spectrometry analysis of nanoscale specimen volumes. Here, we describe a spatially resolved proteomics method based on the combination of tissue expansion with mass spectrometry-based proteomics, which we call Expansion Proteomics (ProteomEx). ProteomEx enables quantitative profiling of the spatial variability of the proteome in mammalian tissues at ~160 µm lateral resolution, equivalent to the tissue volume of 0.61 nL, using manual microsampling without the need for custom or special equipment. We validated and demonstrated the utility of ProteomEx for streamlined large-scale proteomics profiling of biological tissues including brain, liver, and breast cancer. We further applied ProteomEx for identifying proteins associated with Alzheimer's disease in a mouse model by comparative proteomic analysis of brain subregions.
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Affiliation(s)
- Lu Li
- grid.494629.40000 0004 8008 9315Research Center for Industries of the Future and School of Life Sciences, Westlake University, 600 Dunyu Road, Hangzhou, Zhejiang 310030 China ,grid.494629.40000 0004 8008 9315Westlake Laboratory of Life Sciences and Biomedicine, 18 Shilongshan Road, Hangzhou, 310024 Zhejiang China ,grid.494629.40000 0004 8008 9315Key Laboratory of Structural Biology of Zhejiang Province, Westlake University, 18 Shilongshan Road, Hangzhou, 310024 Zhejiang China ,grid.494629.40000 0004 8008 9315Institute of Basic Medical Sciences, Westlake Institute for Advanced Study, 18 Shilongshan Road, Hangzhou, 310024 Zhejiang China ,grid.13402.340000 0004 1759 700XCollege of Pharmaceutical Sciences, Zhejiang University, 866 Yuhangtang Road, Hangzhou, 310024 Zhejiang China
| | - Cuiji Sun
- grid.494629.40000 0004 8008 9315Research Center for Industries of the Future and School of Life Sciences, Westlake University, 600 Dunyu Road, Hangzhou, Zhejiang 310030 China ,grid.494629.40000 0004 8008 9315Westlake Laboratory of Life Sciences and Biomedicine, 18 Shilongshan Road, Hangzhou, 310024 Zhejiang China ,grid.494629.40000 0004 8008 9315Institute of Basic Medical Sciences, Westlake Institute for Advanced Study, 18 Shilongshan Road, Hangzhou, 310024 Zhejiang China
| | - Yaoting Sun
- grid.494629.40000 0004 8008 9315Research Center for Industries of the Future and School of Life Sciences, Westlake University, 600 Dunyu Road, Hangzhou, Zhejiang 310030 China ,grid.494629.40000 0004 8008 9315Westlake Laboratory of Life Sciences and Biomedicine, 18 Shilongshan Road, Hangzhou, 310024 Zhejiang China ,grid.494629.40000 0004 8008 9315Key Laboratory of Structural Biology of Zhejiang Province, Westlake University, 18 Shilongshan Road, Hangzhou, 310024 Zhejiang China ,grid.494629.40000 0004 8008 9315Institute of Basic Medical Sciences, Westlake Institute for Advanced Study, 18 Shilongshan Road, Hangzhou, 310024 Zhejiang China
| | - Zhen Dong
- grid.494629.40000 0004 8008 9315Research Center for Industries of the Future and School of Life Sciences, Westlake University, 600 Dunyu Road, Hangzhou, Zhejiang 310030 China ,grid.494629.40000 0004 8008 9315Westlake Laboratory of Life Sciences and Biomedicine, 18 Shilongshan Road, Hangzhou, 310024 Zhejiang China ,grid.494629.40000 0004 8008 9315Key Laboratory of Structural Biology of Zhejiang Province, Westlake University, 18 Shilongshan Road, Hangzhou, 310024 Zhejiang China ,grid.494629.40000 0004 8008 9315Institute of Basic Medical Sciences, Westlake Institute for Advanced Study, 18 Shilongshan Road, Hangzhou, 310024 Zhejiang China
| | - Runxin Wu
- grid.494629.40000 0004 8008 9315Research Center for Industries of the Future and School of Life Sciences, Westlake University, 600 Dunyu Road, Hangzhou, Zhejiang 310030 China ,grid.494629.40000 0004 8008 9315Westlake Laboratory of Life Sciences and Biomedicine, 18 Shilongshan Road, Hangzhou, 310024 Zhejiang China ,grid.494629.40000 0004 8008 9315Key Laboratory of Structural Biology of Zhejiang Province, Westlake University, 18 Shilongshan Road, Hangzhou, 310024 Zhejiang China ,grid.494629.40000 0004 8008 9315Institute of Basic Medical Sciences, Westlake Institute for Advanced Study, 18 Shilongshan Road, Hangzhou, 310024 Zhejiang China ,grid.21107.350000 0001 2171 9311Whiting School of Engineering, Department of Biomedical Engineering, Johns Hopkins University, Baltimore, MD 21218 USA
| | - Xiaoting Sun
- grid.494629.40000 0004 8008 9315Research Center for Industries of the Future and School of Life Sciences, Westlake University, 600 Dunyu Road, Hangzhou, Zhejiang 310030 China ,grid.494629.40000 0004 8008 9315Westlake Laboratory of Life Sciences and Biomedicine, 18 Shilongshan Road, Hangzhou, 310024 Zhejiang China ,grid.494629.40000 0004 8008 9315Institute of Basic Medical Sciences, Westlake Institute for Advanced Study, 18 Shilongshan Road, Hangzhou, 310024 Zhejiang China
| | - Hanbin Zhang
- grid.494629.40000 0004 8008 9315Research Center for Industries of the Future and School of Life Sciences, Westlake University, 600 Dunyu Road, Hangzhou, Zhejiang 310030 China ,grid.494629.40000 0004 8008 9315Westlake Laboratory of Life Sciences and Biomedicine, 18 Shilongshan Road, Hangzhou, 310024 Zhejiang China ,grid.494629.40000 0004 8008 9315Institute of Basic Medical Sciences, Westlake Institute for Advanced Study, 18 Shilongshan Road, Hangzhou, 310024 Zhejiang China
| | - Wenhao Jiang
- grid.494629.40000 0004 8008 9315Research Center for Industries of the Future and School of Life Sciences, Westlake University, 600 Dunyu Road, Hangzhou, Zhejiang 310030 China ,grid.494629.40000 0004 8008 9315Westlake Laboratory of Life Sciences and Biomedicine, 18 Shilongshan Road, Hangzhou, 310024 Zhejiang China ,grid.494629.40000 0004 8008 9315Key Laboratory of Structural Biology of Zhejiang Province, Westlake University, 18 Shilongshan Road, Hangzhou, 310024 Zhejiang China ,grid.494629.40000 0004 8008 9315Institute of Basic Medical Sciences, Westlake Institute for Advanced Study, 18 Shilongshan Road, Hangzhou, 310024 Zhejiang China
| | - Yan Zhou
- grid.494629.40000 0004 8008 9315Research Center for Industries of the Future and School of Life Sciences, Westlake University, 600 Dunyu Road, Hangzhou, Zhejiang 310030 China ,grid.494629.40000 0004 8008 9315Westlake Laboratory of Life Sciences and Biomedicine, 18 Shilongshan Road, Hangzhou, 310024 Zhejiang China ,grid.494629.40000 0004 8008 9315Key Laboratory of Structural Biology of Zhejiang Province, Westlake University, 18 Shilongshan Road, Hangzhou, 310024 Zhejiang China ,grid.494629.40000 0004 8008 9315Institute of Basic Medical Sciences, Westlake Institute for Advanced Study, 18 Shilongshan Road, Hangzhou, 310024 Zhejiang China
| | - Xufeng Cen
- grid.13402.340000 0004 1759 700XDepartment of Biochemistry & Molecular Medical Center, Zhejiang University School of Medicine, Hangzhou, 310058 China
| | - Shang Cai
- grid.494629.40000 0004 8008 9315Research Center for Industries of the Future and School of Life Sciences, Westlake University, 600 Dunyu Road, Hangzhou, Zhejiang 310030 China ,grid.494629.40000 0004 8008 9315Westlake Laboratory of Life Sciences and Biomedicine, 18 Shilongshan Road, Hangzhou, 310024 Zhejiang China
| | - Hongguang Xia
- grid.13402.340000 0004 1759 700XDepartment of Biochemistry & Molecular Medical Center, Zhejiang University School of Medicine, Hangzhou, 310058 China ,grid.452661.20000 0004 1803 6319Research Center for Clinical Pharmacy & Key Laboratory for Drug Evaluation and Clinical Research of Zhejiang Province, The First Affiliated Hospital, Zhejiang University School of Medicine, Hangzhou, 310003 China ,grid.13402.340000 0004 1759 700XZhejiang Laboratory for Systems & Precision Medicine, Zhejiang University Medical Center, 1369 West Wenyi Road, Hangzhou, 311121 China
| | - Yi Zhu
- grid.494629.40000 0004 8008 9315Research Center for Industries of the Future and School of Life Sciences, Westlake University, 600 Dunyu Road, Hangzhou, Zhejiang 310030 China ,grid.494629.40000 0004 8008 9315Westlake Laboratory of Life Sciences and Biomedicine, 18 Shilongshan Road, Hangzhou, 310024 Zhejiang China ,grid.494629.40000 0004 8008 9315Key Laboratory of Structural Biology of Zhejiang Province, Westlake University, 18 Shilongshan Road, Hangzhou, 310024 Zhejiang China ,grid.494629.40000 0004 8008 9315Institute of Basic Medical Sciences, Westlake Institute for Advanced Study, 18 Shilongshan Road, Hangzhou, 310024 Zhejiang China
| | - Tiannan Guo
- grid.494629.40000 0004 8008 9315Research Center for Industries of the Future and School of Life Sciences, Westlake University, 600 Dunyu Road, Hangzhou, Zhejiang 310030 China ,grid.494629.40000 0004 8008 9315Westlake Laboratory of Life Sciences and Biomedicine, 18 Shilongshan Road, Hangzhou, 310024 Zhejiang China ,grid.494629.40000 0004 8008 9315Key Laboratory of Structural Biology of Zhejiang Province, Westlake University, 18 Shilongshan Road, Hangzhou, 310024 Zhejiang China ,grid.494629.40000 0004 8008 9315Institute of Basic Medical Sciences, Westlake Institute for Advanced Study, 18 Shilongshan Road, Hangzhou, 310024 Zhejiang China
| | - Kiryl D. Piatkevich
- grid.494629.40000 0004 8008 9315Research Center for Industries of the Future and School of Life Sciences, Westlake University, 600 Dunyu Road, Hangzhou, Zhejiang 310030 China ,grid.494629.40000 0004 8008 9315Westlake Laboratory of Life Sciences and Biomedicine, 18 Shilongshan Road, Hangzhou, 310024 Zhejiang China ,grid.494629.40000 0004 8008 9315Institute of Basic Medical Sciences, Westlake Institute for Advanced Study, 18 Shilongshan Road, Hangzhou, 310024 Zhejiang China
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9
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Harkin C, Smith KW, Cruickshank FL, Logan Mackay C, Flinders B, Heeren RMA, Moore T, Brockbank S, Cobice DF. On-tissue chemical derivatization in mass spectrometry imaging. MASS SPECTROMETRY REVIEWS 2022; 41:662-694. [PMID: 33433028 PMCID: PMC9545000 DOI: 10.1002/mas.21680] [Citation(s) in RCA: 44] [Impact Index Per Article: 22.0] [Reference Citation Analysis] [Abstract] [Key Words] [MESH Headings] [Track Full Text] [Subscribe] [Scholar Register] [Received: 09/17/2020] [Revised: 12/03/2020] [Accepted: 12/15/2020] [Indexed: 05/04/2023]
Abstract
Mass spectrometry imaging (MSI) combines molecular and spatial information in a valuable tool for a wide range of applications. Matrix-assisted laser desorption/ionization (MALDI) is at the forefront of MSI ionization due to its wide availability and increasing improvement in spatial resolution and analysis speed. However, ionization suppression, low concentrations, and endogenous and methodological interferences cause visualization problems for certain molecules. Chemical derivatization (CD) has proven a viable solution to these issues when applied in mass spectrometry platforms. Chemical tagging of target analytes with larger, precharged moieties aids ionization efficiency and removes analytes from areas of potential isobaric interferences. Here, we address the application of CD on tissue samples for MSI analysis, termed on-tissue chemical derivatization (OTCD). MALDI MSI will remain the focus platform due to its popularity, however, alternative ionization techniques such as liquid extraction surface analysis and desorption electrospray ionization will also be recognized. OTCD reagent selection, application, and optimization methods will be discussed in detail. MSI with OTCD is a powerful tool to study the spatial distribution of poorly ionizable molecules within tissues. Most importantly, the use of OTCD-MSI facilitates the analysis of previously inaccessible biologically relevant molecules through the adaptation of existing CD methods. Though further experimental optimization steps are necessary, the benefits of this technique are extensive.
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Affiliation(s)
- Carla Harkin
- Mass Spectrometry Centre, Biomedical Sciences Research Institute (BMSRI), School of Biomedical SciencesUlster UniversityColeraineNorthern IrelandUK
| | - Karl W. Smith
- National High Magnetic Field Laboratory, Ion Cyclotron Resonance Facility (ICR)Florida State UniversityTallahasseeFloridaUSA
| | - Faye L. Cruickshank
- Scottish Instrumentation and Research Centre for Advanced Mass Spectrometry (SIRCAMS), EaStCHEM School of ChemistryUniversity of EdinburghScotlandUK
| | - C. Logan Mackay
- Scottish Instrumentation and Research Centre for Advanced Mass Spectrometry (SIRCAMS), EaStCHEM School of ChemistryUniversity of EdinburghScotlandUK
| | - Bryn Flinders
- Screening Division, Mass Spectrometry, Hair DiagnostixDutch Screening GroupMaastrichtThe Netherlands
| | - Ron M. A. Heeren
- Maastricht Multimodal Molecular Imaging Institute (M4I)University of MaastrichtMaastrichtThe Netherlands
| | - Tara Moore
- Genomic Medicine, Biomedical Sciences Research Institute (BMSRI), School of Biomedical SciencesUlster UniversityColeraineNorthern IrelandUK
| | | | - Diego F. Cobice
- Mass Spectrometry Centre, Biomedical Sciences Research Institute (BMSRI), School of Biomedical SciencesUlster UniversityColeraineNorthern IrelandUK
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10
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Hale O, Hughes JW, Sisley EK, Cooper HJ. Native Ambient Mass Spectrometry Enables Analysis of Intact Endogenous Protein Assemblies up to 145 kDa Directly from Tissue. Anal Chem 2022; 94:5608-5614. [PMID: 35358391 PMCID: PMC9008691 DOI: 10.1021/acs.analchem.1c05353] [Citation(s) in RCA: 16] [Impact Index Per Article: 8.0] [Reference Citation Analysis] [Abstract] [MESH Headings] [Grants] [Track Full Text] [Download PDF] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Received: 12/10/2021] [Accepted: 02/22/2022] [Indexed: 02/07/2023]
Abstract
Untargeted label-free interrogation of proteins in their functional form directly from their physiological environment promises to transform life sciences research by providing unprecedented insight into their transient interactions with other biomolecules and xenobiotics. Native ambient mass spectrometry (NAMS) shows great potential for the structural analysis of endogenous protein assemblies directly from tissues; however, to date, this has been limited to assemblies of low molecular weight (<20 kDa) or very high abundance (hemoglobin tetramer in blood vessels, RidA homotrimer in kidney cortex tissues). The present work constitutes a step change for NAMS of protein assemblies: we demonstrate the detection and identification of a range of intact endogenous protein assemblies with various stoichiometries (dimer, trimer, and tetramer) from a range of tissue types (brain, kidney, liver) by the use of multiple NAMS techniques. Crucially, we demonstrate a greater than twofold increase in accessible molecular weight (up to 145 kDa). In addition, spatial distributions of protein assemblies up to 94 kDa were mapped in brain and kidney by nanospray desorption electrospray ionization (nano-DESI) mass spectrometry imaging.
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Affiliation(s)
- Oliver
J. Hale
- School of Biosciences, University of Birmingham, Edgbaston, Birmingham B15 2TT, U.K.
| | - James W. Hughes
- School of Biosciences, University of Birmingham, Edgbaston, Birmingham B15 2TT, U.K.
| | - Emma K. Sisley
- School of Biosciences, University of Birmingham, Edgbaston, Birmingham B15 2TT, U.K.
| | - Helen J. Cooper
- School of Biosciences, University of Birmingham, Edgbaston, Birmingham B15 2TT, U.K.
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11
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Sisley EK, Hale OJ, Styles IB, Cooper HJ. Native Ambient Mass Spectrometry Imaging of Ligand-Bound and Metal-Bound Proteins in Rat Brain. J Am Chem Soc 2022; 144:2120-2128. [DOI: 10.1021/jacs.1c10032] [Citation(s) in RCA: 11] [Impact Index Per Article: 5.5] [Reference Citation Analysis] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Indexed: 12/18/2022]
Affiliation(s)
- Emma K. Sisley
- School of Biosciences, University of Birmingham, Birmingham, B15 2TT, U.K
| | - Oliver J. Hale
- School of Biosciences, University of Birmingham, Birmingham, B15 2TT, U.K
| | - Iain B. Styles
- School of Computer Science, University of Birmingham, Birmingham, B15 2TT, U.K
- The Alan Turing Institute, London, NW1 2DB, U.K
- Centre of Membrane Proteins and Receptors (COMPARE), University of Birmingham, Birmingham, B15 2TT, U.K
- University of Nottingham, Midlands, NG7 2RD, U.K
| | - Helen J. Cooper
- School of Biosciences, University of Birmingham, Birmingham, B15 2TT, U.K
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12
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Olajide OE, Donkor B, Hamid AM. Systematic Optimization of Ambient Ionization Ion Mobility Mass Spectrometry for Rapid Separation of Isomers. JOURNAL OF THE AMERICAN SOCIETY FOR MASS SPECTROMETRY 2022; 33:160-171. [PMID: 34910491 DOI: 10.1021/jasms.1c00311] [Citation(s) in RCA: 6] [Impact Index Per Article: 3.0] [Reference Citation Analysis] [Abstract] [Key Words] [Track Full Text] [Subscribe] [Scholar Register] [Indexed: 06/14/2023]
Abstract
Current methods typically used for metabolite screening and disease diagnosis often require extensive sample preparation, which increases analysis time and associated costs. While ambient ionization techniques enable the analysis of various samples in complex matrices with little or no sample preparation in a short time (typically within a minute), their reduced selectivity, even when coupled with high-resolution mass spectrometers, limits their application in certain fields. In this study, we have optimized the coupling of paper spray (PS) and leaf spray (LS) ambient ionization techniques with a commercially available ion mobility mass spectrometer (IM-MS) and demonstrated the separation of geometric and constitutional isomers. Ambient ionization techniques allow simultaneous introduction and ionization of samples, while background noise and matrix interference from paper and leaf substrates are filtered out by IM separation, resulting in high sensitivity and selectivity of the PS-IM-MS and LS-IM-MS workflows. In addition, we introduced a novel approach to perform single-field collision cross section (CCS) measurements, which resulted in CCS values that differ by 0.15% and 0.25% from traditional stepped-field and single-field methods, respectively. In addition, we used advanced computational tools to confidently identify analyte structures by comparing CCS values from experimental IM measurements and theoretical calculations. These results suggest that the coupling of ambient ionization methods with ion mobility techniques enables rapid, sensitive, and highly selective analysis that can be used in different fields, such as agrochemical screening and disease diagnostics.
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Affiliation(s)
- Orobola E Olajide
- Department of Chemistry and Biochemistry, Auburn University, Auburn, Alabama 36849-5312, United States
| | - Benedicta Donkor
- Department of Chemistry and Biochemistry, Auburn University, Auburn, Alabama 36849-5312, United States
| | - Ahmed M Hamid
- Department of Chemistry and Biochemistry, Auburn University, Auburn, Alabama 36849-5312, United States
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13
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Otsuka Y. Direct Liquid Extraction and Ionization Techniques for Understanding Multimolecular Environments in Biological Systems (Secondary Publication). Mass Spectrom (Tokyo) 2021; 10:A0095. [PMID: 34249586 PMCID: PMC8246329 DOI: 10.5702/massspectrometry.a0095] [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: 04/20/2021] [Accepted: 04/21/2021] [Indexed: 11/23/2022] Open
Abstract
A combination of direct liquid extraction using a small volume of solvent and electrospray ionization allows the rapid measurement of complex chemical components in biological samples and visualization of their distribution in tissue sections. This review describes the development of such techniques and their application to biological research since the first reports in the early 2000s. An overview of electrospray ionization, ion suppression in samples, and the acceleration of specific chemical reactions in charged droplets is also presented. Potential future applications for visualizing multimolecular environments in biological systems are discussed.
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Affiliation(s)
- Yoichi Otsuka
- Graduate School of Science, Osaka University, 1–1 Machikaneyama-cho, Toyonaka, Osaka 560–0043, Japan
- JST, PRESTO, 4–1–8 Honcho, Kawaguchi, Saitama 332–0012, Japan
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14
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Smythers AL, Hicks LM. Mapping the plant proteome: tools for surveying coordinating pathways. Emerg Top Life Sci 2021; 5:203-220. [PMID: 33620075 PMCID: PMC8166341 DOI: 10.1042/etls20200270] [Citation(s) in RCA: 6] [Impact Index Per Article: 2.0] [Reference Citation Analysis] [Abstract] [Key Words] [MESH Headings] [Track Full Text] [Download PDF] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Received: 01/04/2021] [Revised: 02/07/2021] [Accepted: 02/09/2021] [Indexed: 12/14/2022]
Abstract
Plants rapidly respond to environmental fluctuations through coordinated, multi-scalar regulation, enabling complex reactions despite their inherently sessile nature. In particular, protein post-translational signaling and protein-protein interactions combine to manipulate cellular responses and regulate plant homeostasis with precise temporal and spatial control. Understanding these proteomic networks are essential to addressing ongoing global crises, including those of food security, rising global temperatures, and the need for renewable materials and fuels. Technological advances in mass spectrometry-based proteomics are enabling investigations of unprecedented depth, and are increasingly being optimized for and applied to plant systems. This review highlights recent advances in plant proteomics, with an emphasis on spatially and temporally resolved analysis of post-translational modifications and protein interactions. It also details the necessity for generation of a comprehensive plant cell atlas while highlighting recent accomplishments within the field.
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Affiliation(s)
- Amanda L Smythers
- Department of Chemistry, The University of North Carolina at Chapel Hill, Chapel Hill, NC 27599, U.S.A
| | - Leslie M Hicks
- Department of Chemistry, The University of North Carolina at Chapel Hill, Chapel Hill, NC 27599, U.S.A
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15
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Fulcher JM, Makaju A, Moore RJ, Zhou M, Bennett DA, De Jager PL, Qian WJ, Paša-Tolić L, Petyuk VA. Enhancing Top-Down Proteomics of Brain Tissue with FAIMS. J Proteome Res 2021; 20:2780-2795. [PMID: 33856812 PMCID: PMC8672206 DOI: 10.1021/acs.jproteome.1c00049] [Citation(s) in RCA: 31] [Impact Index Per Article: 10.3] [Reference Citation Analysis] [Abstract] [Key Words] [MESH Headings] [Grants] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Indexed: 01/12/2023]
Abstract
Proteomic investigations of Alzheimer's and Parkinson's disease have provided valuable insights into neurodegenerative disorders. Thus far, these investigations have largely been restricted to bottom-up approaches, hindering the degree to which one can characterize a protein's "intact" state. Top-down proteomics (TDP) overcomes this limitation; however, it is typically limited to observing only the most abundant proteoforms and of a relatively small size. Therefore, fractionation techniques are commonly used to reduce sample complexity. Here, we investigate gas-phase fractionation through high-field asymmetric waveform ion mobility spectrometry (FAIMS) within TDP. Utilizing a high complexity sample derived from Alzheimer's disease (AD) brain tissue, we describe how the addition of FAIMS to TDP can robustly improve the depth of proteome coverage. For example, implementation of FAIMS with external compensation voltage (CV) stepping at -50, -40, and -30 CV could more than double the mean number of non-redundant proteoforms, genes, and proteome sequence coverage compared to without FAIMS. We also found that FAIMS can influence the transmission of proteoforms and their charge envelopes based on their size. Importantly, FAIMS enabled the identification of intact amyloid beta (Aβ) proteoforms, including the aggregation-prone Aβ1-42 variant which is strongly linked to AD. Raw data and associated files have been deposited to the ProteomeXchange Consortium via the MassIVE data repository with data set identifier PXD023607.
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Affiliation(s)
- James M Fulcher
- Biological Sciences Division, Pacific Northwest National Laboratory, Richland, Washington 99352, United States
| | - Aman Makaju
- Life Sciences Mass Spectrometry Unit, Thermo Fisher Scientific, San Jose, California 95134, United States
| | - Ronald J Moore
- Biological Sciences Division, Pacific Northwest National Laboratory, Richland, Washington 99352, United States
| | - Mowei Zhou
- Environmental Molecular Sciences Laboratory, Pacific Northwest National Laboratory, Richland, Washington 99354, United States
| | - David A Bennett
- Rush Alzheimer's Disease Center, Rush University Medical Center, Chicago, Illinois 60612, United States
| | - Philip L De Jager
- Department of Neurology, Center for Translational & Computational Neuroimmunology, Columbia University Medical Center, New York, New York 10032, United States
| | - Wei-Jun Qian
- Biological Sciences Division, Pacific Northwest National Laboratory, Richland, Washington 99352, United States
| | - Ljiljana Paša-Tolić
- Environmental Molecular Sciences Laboratory, Pacific Northwest National Laboratory, Richland, Washington 99354, United States
| | - Vladislav A Petyuk
- Biological Sciences Division, Pacific Northwest National Laboratory, Richland, Washington 99352, United States
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16
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Gerbasi VR, Melani RD, Abbatiello SE, Belford MW, Huguet R, McGee JP, Dayhoff D, Thomas PM, Kelleher NL. Deeper Protein Identification Using Field Asymmetric Ion Mobility Spectrometry in Top-Down Proteomics. Anal Chem 2021; 93:6323-6328. [PMID: 33844503 DOI: 10.1021/acs.analchem.1c00402] [Citation(s) in RCA: 33] [Impact Index Per Article: 11.0] [Reference Citation Analysis] [Abstract] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Indexed: 12/17/2022]
Abstract
Field asymmetric ion mobility spectrometry (FAIMS), when used in proteomics studies, provides superior selectivity and enables more proteins to be identified by providing additional gas-phase separation. Here, we tested the performance of cylindrical FAIMS for the identification and characterization of proteoforms by top-down mass spectrometry of heterogeneous protein mixtures. Combining FAIMS with chromatographic separation resulted in a 62% increase in protein identifications, an 8% increase in proteoform identifications, and an improvement in proteoform identification compared to samples analyzed without FAIMS. In addition, utilization of FAIMS resulted in the identification of proteins encoded by lower-abundance mRNA transcripts. These improvements were attributable, in part, to improved signal-to-noise for proteoforms with similar retention times. Additionally, our results show that the optimal compensation voltage of any given proteoform was correlated with the molecular weight of the analyte. Collectively these results suggest that the addition of FAIMS can enhance top-down proteomics in both discovery and targeted applications.
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Affiliation(s)
- Vincent R Gerbasi
- Northwestern University, National Resource for Translational and Developmental Proteomics, Evanston, Illinois 60208, United States.,Pacific Northwest National Laboratories, Richland, Washington 99352, United States
| | - Rafael D Melani
- Northwestern University, National Resource for Translational and Developmental Proteomics, Evanston, Illinois 60208, United States
| | - Susan E Abbatiello
- Northeastern University, Boston, Massachusetts 02115, United States.,Thermo Fisher Scientific, San Jose, California 98665, United States
| | | | - Romain Huguet
- Thermo Fisher Scientific, San Jose, California 98665, United States
| | - John P McGee
- Northwestern University, National Resource for Translational and Developmental Proteomics, Evanston, Illinois 60208, United States
| | - Dawson Dayhoff
- Northwestern University, National Resource for Translational and Developmental Proteomics, Evanston, Illinois 60208, United States
| | - Paul M Thomas
- Northwestern University, National Resource for Translational and Developmental Proteomics, Evanston, Illinois 60208, United States
| | - Neil L Kelleher
- Northwestern University, National Resource for Translational and Developmental Proteomics, Evanston, Illinois 60208, United States
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17
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Xiao Y, Deng J, Fang L, Tu L, Luan T. Mapping the distribution of perfluoroalkyl substances in zebrafishes by liquid extraction surface analysis mass spectrometry. Talanta 2021; 231:122377. [PMID: 33965041 DOI: 10.1016/j.talanta.2021.122377] [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: 12/24/2020] [Revised: 03/24/2021] [Accepted: 03/27/2021] [Indexed: 10/21/2022]
Abstract
Investigation on the distribution of persistent organic pollutants (POPs) in aquatic organisms is of great importance for exploring the biological toxicity and health risks of environmental pollutants. In this study, a liquid extraction surface analysis mass spectrometry (LESA-MS) method was developed for rapid and in situ analysis of the spatial distribution of perfluoroalkyl substances (PFASs) in zebrafish. By combining the high-precision automated moving platform of LESA device and the high-resolution MS, quantitative analysis of perfluorooctanoic acid (PFOA) and perfluorooctanesulfonic acid (PFOS) in zebrafish tissue section were easily achieved. A tissue-specific ionization efficiency factor (TSF) strategy was also proposed to correct the matrix effect in different parts of zebrafish tissue. By using the developed method, high sensitive and efficient imaging of PFOA and PFOS in zebrafish tissue was achieved, and the distributions of PFOA and PFOS in descending order were gills, organs, roes, pelvic fin, muscle, and brain. The experimental results demonstrated that the coupling of LESA-MS method with TFS strategy is an efficient and reliable approach for monitoring the content distribution of environmental pollutants in biological tissues.
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Affiliation(s)
- Yipo Xiao
- State Key Laboratory of Biocontrol, South China Sea Bio-Resource Exploitation and Utilization Collaborative Innovation Center, School of Life Sciences, Sun Yat-Sen University, 135 Xingangxi Road, Guangzhou, 510275, China
| | - Jiewei Deng
- School of Biomedical and Pharmaceutical Sciences, Guangdong University of Technology, 100 Waihuanxi Road, Guangzhou, 510006, China.
| | - Ling Fang
- State Key Laboratory of Biocontrol, South China Sea Bio-Resource Exploitation and Utilization Collaborative Innovation Center, School of Life Sciences, Sun Yat-Sen University, 135 Xingangxi Road, Guangzhou, 510275, China
| | - Lanyin Tu
- State Key Laboratory of Biocontrol, South China Sea Bio-Resource Exploitation and Utilization Collaborative Innovation Center, School of Life Sciences, Sun Yat-Sen University, 135 Xingangxi Road, Guangzhou, 510275, China
| | - Tiangang Luan
- State Key Laboratory of Biocontrol, South China Sea Bio-Resource Exploitation and Utilization Collaborative Innovation Center, School of Life Sciences, Sun Yat-Sen University, 135 Xingangxi Road, Guangzhou, 510275, China; Institute of Environmental and Ecological Engineering, Guangdong University of Technology, 100 Waihuanxi Road, Guangzhou, 510006, China.
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18
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Chen CL, Kuo TH, Chung HH, Huang P, Lin LE, Hsu CC. Remodeling nanoDESI Platform with Ion Mobility Spectrometry to Expand Protein Coverage in Cancerous Tissue. JOURNAL OF THE AMERICAN SOCIETY FOR MASS SPECTROMETRY 2021; 32:653-660. [PMID: 33507077 DOI: 10.1021/jasms.0c00354] [Citation(s) in RCA: 10] [Impact Index Per Article: 3.3] [Reference Citation Analysis] [Abstract] [Key Words] [MESH Headings] [Track Full Text] [Subscribe] [Scholar Register] [Indexed: 06/12/2023]
Abstract
Nanospray desorption electrospray ionization mass spectrometry is an ambient ionization technique that is capable of mapping proteins in tissue sections. However, high-abundant molecules or isobaric interference in biological samples hampers its broad applications in probing low-abundant proteins. To address this challenge, herein we demonstrated an integrated module that coupled pneumatic-assisted nanospray desorption electrospray ionization mass spectrometry with high-field asymmetric ion mobility spectrometry. Using this module to analyze mouse brain sections, the protein coverage was significantly increased. This improvement allowed the mapping of low-abundant proteins in tissue sections with a 5 μm spatial resolution enabled by computationally assisted fusion with optical microscopic images. Moreover, the module was successfully applied to characterize melanoma in skin tissues based on the enhanced protein profiles. The results suggested that this integrating module will be potentially applied to discover novel proteins in cancers.
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Affiliation(s)
- Chih-Lin Chen
- Department of Chemistry, National Taiwan University, Taipei 106216, Taiwan
| | - Ting-Hao Kuo
- Department of Chemistry, National Taiwan University, Taipei 106216, Taiwan
| | - Hsin-Hsiang Chung
- Department of Chemistry, National Taiwan University, Taipei 106216, Taiwan
| | - Penghsuan Huang
- Department of Chemistry, National Taiwan University, Taipei 106216, Taiwan
| | - Li-En Lin
- Department of Chemistry, National Taiwan University, Taipei 106216, Taiwan
| | - Cheng-Chih Hsu
- Department of Chemistry, National Taiwan University, Taipei 106216, Taiwan
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19
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Cintron-Diaz YL, Acanda de la Rocha AM, Castellanos A, Chambers JM, Fernandez-Lima F. Mapping chemotherapeutic drug distribution in cancer cell spheroids using 2D-TOF-SIMS and LESA-TIMS-MS. Analyst 2020; 145:7056-7062. [PMID: 32966375 DOI: 10.1039/c9an02245g] [Citation(s) in RCA: 2] [Impact Index Per Article: 0.5] [Reference Citation Analysis] [Abstract] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Indexed: 11/21/2022]
Abstract
Three-dimensional (3D) cancer cell cultures grown in the form of spheroids are effective models for the study of in vivo-like processes simulating cancer tumor pharmacological dynamics and morphology. In this study, we show the advantages of Time-of-Flight Secondary Ion Mass Spectrometry (TOF-SIMS) combined with in situ Liquid Extraction Surface Analysis coupled to trapped Ion Mobility Spectrometry Mass Spectrometry (LESA-TIMS-TOF MS) for high spatial resolution mapping and quantitation of ABT-737, a chemotherapeutic drug, at the level of single human colon carcinoma cell spheroids (HCT 116 MCS). 2D-TOF-SIMS studies of consecutive sections (∼16 μm thick slices) showed that ABT-737 is homogenously distributed in the outer layers of the HCT 116 MCS. Complementary in situ LESA-TIMS-TOF MS/MS measurements confirmed the presence of the ABT-737 drug in the MCS slides by the observation of the molecular ion [M + H]+m/z and mobility, and the charateristic fragmentation pattern. LESA-TIMS-TOF MS allowed a quantitative assessment of the ABT-737 drug of the control MCS slice spiked with ABT-737 standard over the 0.4-4.1 ng range and MCS treated starting at 10 μM for 24 h. These experiments showcase an effective protocol for unambigous characterization and 3D mapping of chemotherapeutic drug distribution at the single MCS level.
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Affiliation(s)
- Yarixa L Cintron-Diaz
- Department of Chemistry and Biochemistry, Florida International University, 11200 SW 8th St., AHC4-233, Miami, FL 33199, USA.
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20
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Muraki N, Takano H, Akiyama T. Study of oxygenation and hydrogenation of tris(8-hydroxyquinoline) aluminum generated by electrode deposition using liquid extraction surface analysis nanoelectrospray ionization mass spectrometry. Chem Phys Lett 2020. [DOI: 10.1016/j.cplett.2020.137791] [Citation(s) in RCA: 0] [Impact Index Per Article: 0] [Reference Citation Analysis] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Indexed: 11/29/2022]
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21
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Chen B, Vavrek M, Gundersdorf R, Zhong W, Cancilla MT. Combining MALDI mass spectrometry imaging and droplet-base surface sampling analysis for tissue distribution, metabolite profiling, and relative quantification of cyclic peptide melanotan II. Anal Chim Acta 2020; 1125:279-287. [PMID: 32674774 DOI: 10.1016/j.aca.2020.05.050] [Citation(s) in RCA: 6] [Impact Index Per Article: 1.5] [Reference Citation Analysis] [Abstract] [Key Words] [MESH Headings] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Received: 02/21/2020] [Revised: 04/30/2020] [Accepted: 05/21/2020] [Indexed: 12/21/2022]
Abstract
Peptides have become a fast-growing segment of the pharmaceutical industry over the past few decades. It is essential to develop cutting edge analytical techniques to support the discovery and development of peptide therapeutics, especially to examine their absorption, distribution, metabolism and excretion (ADME) properties. Herein, we utilized two label-free mass spectrometry (MS) based techniques to investigate representative challenges in developing therapeutic peptides, such as tissue distribution, metabolic stability and clearance. A tool proof-of-concept cyclic peptide, melanotan II, was used in this study. Matrix-assisted laser desorption/ionization mass spectrometry imaging (MALDI-MSI), which is a well-developed label-free imaging technique, was used to map the detailed molecular distribution of melanotan II and its metabolites. Droplet-based liquid microjunction surface sampling liquid chromatography-high resolution mass spectrometry (LMJ-SSP-LC-HRMS) was used in combination with MALDI-MSI to rapidly profile molecular information and provide structural insights on drug and metabolites. Using both techniques in parallel allowed a more comprehensive and complementary data set than using either technique independently. We envision MALDI-MSI and droplet-based LMJ-SSP-LC-HRMS, which can be used in combination or as standalone techniques, to become valuable tools for assessing the in vivo fate of peptide therapeutics in support of drug discovery and development.
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Affiliation(s)
- Bingming Chen
- Department of Pharmacokinetics, Pharmacodynamics & Drug Metabolism (PPDM), Merck & Co., Inc., 2000 Galloping Hill Rd, Kenilworth, NJ, 07033, USA.
| | - Marissa Vavrek
- Department of Pharmacokinetics, Pharmacodynamics & Drug Metabolism (PPDM), Merck & Co., Inc., 2000 Galloping Hill Rd, Kenilworth, NJ, 07033, USA
| | - Richard Gundersdorf
- Department of Pharmacokinetics, Pharmacodynamics & Drug Metabolism (PPDM), Merck & Co., Inc., 2000 Galloping Hill Rd, Kenilworth, NJ, 07033, USA
| | - Wendy Zhong
- Analytical Research & Development, Merck & Co., Inc., 2000 Galloping Hill Rd, Kenilworth, NJ, 07033, USA
| | - Mark T Cancilla
- Department of Pharmacokinetics, Pharmacodynamics & Drug Metabolism (PPDM), Merck & Co., Inc., 2000 Galloping Hill Rd, Kenilworth, NJ, 07033, USA.
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22
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Waas M, Kislinger T. Addressing Cellular Heterogeneity in Cancer through Precision Proteomics. J Proteome Res 2020; 19:3607-3619. [PMID: 32697918 DOI: 10.1021/acs.jproteome.0c00338] [Citation(s) in RCA: 3] [Impact Index Per Article: 0.8] [Reference Citation Analysis] [Abstract] [Key Words] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Indexed: 12/18/2022]
Abstract
Cells exhibit a broad spectrum of functions driven by differences in molecular phenotype. Understanding the heterogeneity between and within cell types has led to advances in our ability to diagnose and manipulate biological systems. Heterogeneity within and between tumors still poses a challenge to the development and efficacy of therapeutics. In this Perspective we review the toolkit of protein-level experimental approaches for investigating cellular heterogeneity. We describe how innovative approaches and technical developments have supported the advent of bottom-up single-cell proteomic analysis and present opportunities and challenges within cancer research. Finally, we introduce the concept of "precision proteomics" and discuss how the advantages and limitations of various experimental approaches render them suitable for different biological systems and questions.
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23
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Havlikova J, May RC, Styles IB, Cooper HJ. Direct identification of bacterial and human proteins from infected wounds in living 3D skin models. Sci Rep 2020; 10:11900. [PMID: 32681099 PMCID: PMC7368034 DOI: 10.1038/s41598-020-68233-6] [Citation(s) in RCA: 11] [Impact Index Per Article: 2.8] [Reference Citation Analysis] [Abstract] [Track Full Text] [Download PDF] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Received: 12/11/2019] [Accepted: 06/19/2020] [Indexed: 11/23/2022] Open
Abstract
Trauma is one of the leading causes of death in people under the age of 49 and complications due to wound infection are the primary cause of death in the first few days after injury. The ESKAPE pathogens are a group of bacteria that are a leading cause of hospital-acquired infections and a major concern in terms of antibiotic resistance. Here, we demonstrate a novel and highly accurate approach for the rapid identification of ESKAPE pathogens (Enterococcus faecium, Staphylococcus aureus, Klebsiella pneumoniae, Acinetobacter baumannii, Pseudomonas aeruginosa, and Enterobacter spp.) directly from infected wounds in 3D in vitro skin models. Wounded skin models were inoculated with bacteria and left to incubate. Bacterial proteins were identified within minutes, directly from the wound, by liquid extraction surface analysis mass spectrometry. This approach was able to distinguish closely related strains and, unlike genomic approaches, can be modified to provide dynamic information about pathogen behaviour at the wound site. In addition, since human skin proteins were also identified, this method offers the opportunity to analyse both host and pathogen biomarkers during wound infection in near real-time.
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Affiliation(s)
- Jana Havlikova
- EPSRC Centre for Doctoral Training in Physical Sciences for Health, University of Birmingham, Edgbaston, Birmingham, B15 2TT, UK.,School of Biosciences, University of Birmingham, Edgbaston, Birmingham, B15 2TT, UK
| | - Robin C May
- School of Biosciences, University of Birmingham, Edgbaston, Birmingham, B15 2TT, UK.,Institute of Microbiology and Infection, University of Birmingham, Edgbaston, Birmingham, B15 2TT, UK
| | - Iain B Styles
- EPSRC Centre for Doctoral Training in Physical Sciences for Health, University of Birmingham, Edgbaston, Birmingham, B15 2TT, UK.,School of Computer Science, University of Birmingham, Edgbaston, Birmingham, B15 2TT, UK.,Centre of Membrane Proteins and Receptors, The Universities of Birmingham and Nottingham, The Midlands, Birmingham, UK.,Alan Turing Institute, 96 Euston Road, London, NW1 2DB, UK
| | - Helen J Cooper
- School of Biosciences, University of Birmingham, Edgbaston, Birmingham, B15 2TT, UK.
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24
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Hale OJ, Illes-Toth E, Mize TH, Cooper HJ. High-Field Asymmetric Waveform Ion Mobility Spectrometry and Native Mass Spectrometry: Analysis of Intact Protein Assemblies and Protein Complexes. Anal Chem 2020; 92:6811-6816. [PMID: 32343119 PMCID: PMC7304667 DOI: 10.1021/acs.analchem.0c00649] [Citation(s) in RCA: 28] [Impact Index Per Article: 7.0] [Reference Citation Analysis] [Abstract] [Track Full Text] [Download PDF] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Indexed: 01/06/2023]
Abstract
![]()
High-field asymmetric
waveform ion mobility spectrometry (FAIMS)
enables the separation of ions on the basis of their differential
mobility in an asymmetric oscillating electric field. We, and others,
have previously demonstrated the benefits of FAIMS for the analysis
of peptides and denatured proteins. To date, FAIMS has not been integrated
with native mass spectrometry of folded proteins and protein complexes,
largely due to concerns over the heating effects associated with the
high electric fields employed. Here, we demonstrate the newly introduced
cylindrical FAIMS Pro device coupled with an Orbitrap Eclipse enables
analysis of intact protein assemblies up to 147 kDa. No evidence for
dissociation was detected suggesting that any field heating is insufficient
to disrupt the noncovalent interactions governing these assemblies.
Moreover, the FAIMS device was integrated into native liquid extraction
surface analysis (LESA) MS of protein assemblies directly from thin
tissue sections. Intact tetrameric hemoglobin (64 kDa) and trimeric
reactive intermediate deiminase A (RidA, 43 kDa) were detected. Improvements
in signal-to-noise of between 1.5× and 12× were observed
for these protein assemblies on integration of FAIMS.
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Affiliation(s)
- Oliver J Hale
- School of Biosciences, University of Birmingham, Edgbaston B15 2TT, U.K
| | - Eva Illes-Toth
- School of Biosciences, University of Birmingham, Edgbaston B15 2TT, U.K
| | - Todd H Mize
- School of Biosciences, University of Birmingham, Edgbaston B15 2TT, U.K
| | - Helen J Cooper
- School of Biosciences, University of Birmingham, Edgbaston B15 2TT, U.K
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25
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Sisley EK, Ujma J, Palmer M, Giles K, Fernandez-Lima FA, Cooper HJ. LESA Cyclic Ion Mobility Mass Spectrometry of Intact Proteins from Thin Tissue Sections. Anal Chem 2020; 92:6321-6326. [PMID: 32271006 PMCID: PMC7304663 DOI: 10.1021/acs.analchem.9b05169] [Citation(s) in RCA: 14] [Impact Index Per Article: 3.5] [Reference Citation Analysis] [Abstract] [Track Full Text] [Download PDF] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Indexed: 12/16/2022]
Abstract
![]()
Liquid
extraction surface analysis (LESA) is an ambient surface
sampling technique that allows the analysis of intact proteins directly
from tissue samples via mass spectrometry. Integration of ion mobility
separation to LESA mass spectrometry workflows has shown significant
improvements in the signal-to-noise ratios of the resulting protein
mass spectra and hence the number of proteins detected. Here, we report
the use of a quadrupole–cyclic ion mobility–time-of-flight
mass spectrometer (Q-cIM-ToF) for the analysis of proteins from mouse
brain and rat kidney tissues sampled via LESA. Among other features,
the instrument allows multiple pass cyclic ion mobility separation,
with concomitant increase in resolving power. Single-pass experiments
enabled the detection of 30 proteins from mouse brain tissue, rising
to 44 when quadrupole isolation was employed. In the absence of ion
mobility separation, 21 proteins were detected in rat kidney tissue
including the abundant α- and β-globin chains from hemoglobin.
Single-pass cyclic ion mobility mass spectrometry enabled the detection
of 60 additional proteins. Multipass experiments of a narrow m/z range (m/z 870–920) resulted in the detection of 24 proteins (one pass),
37 proteins (two passes) and 54 proteins (three passes), thus demonstrating
the benefits of improved mobility resolving power.
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Affiliation(s)
| | - Jakub Ujma
- Waters Corporation, Wilmslow SK9 4AX, United Kingdom
| | - Martin Palmer
- Waters Corporation, Wilmslow SK9 4AX, United Kingdom
| | - Kevin Giles
- Waters Corporation, Wilmslow SK9 4AX, United Kingdom
| | - Francisco A Fernandez-Lima
- Department of Chemistry and Biochemistry, Florida International University, Miami, Florida 33199, United States
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26
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Hale OJ, Sisley EK, Griffiths RL, Styles IB, Cooper HJ. Native LESA TWIMS-MSI: Spatial, Conformational, and Mass Analysis of Proteins and Protein Complexes. JOURNAL OF THE AMERICAN SOCIETY FOR MASS SPECTROMETRY 2020; 31:873-879. [PMID: 32159346 PMCID: PMC7147347 DOI: 10.1021/jasms.9b00122] [Citation(s) in RCA: 24] [Impact Index Per Article: 6.0] [Reference Citation Analysis] [Abstract] [MESH Headings] [Track Full Text] [Subscribe] [Scholar Register] [Received: 12/06/2019] [Revised: 02/13/2020] [Accepted: 02/18/2020] [Indexed: 05/18/2023]
Abstract
We have previously demonstrated native liquid extraction surface analysis (LESA) mass spectrometry imaging of small intact proteins in thin tissue sections. We also showed calculation of collision cross sections for specific proteins extracted from discrete locations in tissue by LESA traveling wave ion mobility spectrometry (TWIMS). Here, we demonstrate an integrated native LESA TWIMS mass spectrometry imaging (MSI) workflow, in which ion mobility separation is central to the imaging experiment and which provides spatial, conformational, and mass information on endogenous proteins in a single experiment. The approach was applied to MSI of a thin tissue section of mouse kidney. The results show that the benefits of integration of TWIMS include improved specificity of the ion images and the capacity to calculate collision cross sections for any protein or protein complex detected in any pixel (without a priori knowledge of the presence of the protein).
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Affiliation(s)
- Oliver J. Hale
- School of Biosciences, University of
Birmingham, Edgbaston B15 2TT, U.K.
| | - Emma K. Sisley
- School of Biosciences, University of
Birmingham, Edgbaston B15 2TT, U.K.
| | - Rian L. Griffiths
- School of Biosciences, University of
Birmingham, Edgbaston B15 2TT, U.K.
| | - Iain B. Styles
- School of Computer Science, University of
Birmingham, Edgbaston B15 2TT, U.K.
| | - Helen J. Cooper
- School of Biosciences, University of
Birmingham, Edgbaston B15 2TT, U.K.
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27
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28
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Hale OJ, Cooper HJ. In situ mass spectrometry analysis of intact proteins and protein complexes from biological substrates. Biochem Soc Trans 2020; 48:317-326. [PMID: 32010951 PMCID: PMC7054757 DOI: 10.1042/bst20190793] [Citation(s) in RCA: 5] [Impact Index Per Article: 1.3] [Reference Citation Analysis] [Abstract] [Key Words] [MESH Headings] [Track Full Text] [Download PDF] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Received: 11/18/2019] [Revised: 01/09/2020] [Accepted: 01/09/2020] [Indexed: 12/15/2022]
Abstract
Advances in sample preparation, ion sources and mass spectrometer technology have enabled the detection and characterisation of intact proteins. The challenges associated include an appropriately soft ionisation event, efficient transmission and detection of the often delicate macromolecules. Ambient ion sources, in particular, offer a wealth of strategies for analysis of proteins from solution environments, and directly from biological substrates. The last two decades have seen rapid development in this area. Innovations include liquid extraction surface analysis, desorption electrospray ionisation and nanospray desorption electrospray ionisation. Similarly, developments in native mass spectrometry allow protein-protein and protein-ligand complexes to be ionised and analysed. Identification and characterisation of these large ions involves a suite of hyphenated mass spectrometry techniques, often including the coupling of ion mobility spectrometry and fragmentation techniques. The latter include collision, electron and photon-induced methods, each with their own characteristics and benefits for intact protein identification. In this review, recent developments for in situ protein analysis are explored, with a focus on ion sources and tandem mass spectrometry techniques used for identification.
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Affiliation(s)
- Oliver J. Hale
- School of Biosciences, University of Birmingham, Edgbaston B15 2TT, U.K
| | - Helen J. Cooper
- School of Biosciences, University of Birmingham, Edgbaston B15 2TT, U.K
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29
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Griffiths RL, Hughes JW, Abbatiello SE, Belford MW, Styles IB, Cooper HJ. Comprehensive LESA Mass Spectrometry Imaging of Intact Proteins by Integration of Cylindrical FAIMS. Anal Chem 2020; 92:2885-2890. [PMID: 31967787 PMCID: PMC7145278 DOI: 10.1021/acs.analchem.9b05124] [Citation(s) in RCA: 29] [Impact Index Per Article: 7.3] [Reference Citation Analysis] [Abstract] [Track Full Text] [Download PDF] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Indexed: 12/15/2022]
Abstract
The benefits of high field asymmetric waveform ion mobility spectrometry (FAIMS) for mass spectrometry imaging of intact proteins in thin tissue sections have been demonstrated previously. In those works, a planar FAIMS device coupled with a Thermo Elite mass spectrometer was employed. Here, we have evaluated a newly introduced cylindrical FAIMS device (the FAIMS Pro) coupled with a Thermo Fusion Lumos mass spectrometer for liquid extraction surface analysis mass spectrometry imaging of intact proteins in thin tissue sections from rat testes, kidney, and brain. The method makes use of multiple FAIMS compensation values at each location (pixel) of the imaging array. A total of 975 nonredundant protein species were detected in the testes imaging dataset, 981 in the kidney dataset, and 249 in the brain dataset. These numbers represent a 7-fold (brain) and over 10-fold (testes, kidney) improvement on the numbers of proteins previously detected in LESA FAIMS imaging, and a 10-fold to over 20-fold improvement on the numbers detected without FAIMS on this higher performance mass spectrometer, approaching the same order of magnitude as those obtained in top-down proteomics of cell lines. Nevertheless, high throughput identification within the LESA FAIMS imaging workflow remains a challenge.
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Affiliation(s)
- Rian L Griffiths
- School of Biosciences , University of Birmingham , Edgbaston , Birmingham B15 2TT , United Kingdom
| | - James W Hughes
- School of Biosciences , University of Birmingham , Edgbaston , Birmingham B15 2TT , United Kingdom.,EPSRC Centre for Doctoral Training in Physical Sciences for Health , University of Birmingham , Birmingham B15 2TT , United Kingdom
| | - Susan E Abbatiello
- Thermo Fisher Scientific , Memorial Drive , Cambridge , Massachusetts 02139 , United States
| | - Michael W Belford
- Thermo Fisher Scientific , River Oaks Parkway , San Jose , California 95134 , United States
| | - Iain B Styles
- School of Computer Sciences , University of Birmingham , Birmingham B15 2TT , United Kingdom
| | - Helen J Cooper
- School of Biosciences , University of Birmingham , Edgbaston , Birmingham B15 2TT , United Kingdom
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30
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Liquid Extraction Surface Analysis (LESA) High-Field Asymmetric Waveform Ion Mobility Spectrometry (FAIMS) Mass Spectrometry for In Situ Analysis of Intact Proteins. Methods Mol Biol 2020; 2084:191-201. [PMID: 31729662 DOI: 10.1007/978-1-0716-0030-6_12] [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: 01/11/2023]
Abstract
Liquid extraction surface analysis (LESA) is an ambient mass spectrometry technique which enables direct analysis of analytes from solid substrates. LESA is particularly suitable for the analysis of intact proteins from biological substrates such as thin tissue sections and bacterial colonies growing on agar. Nevertheless, these substrates present a challenge for LESA protein analysis owing to their inherent complexity. It is therefore beneficial to hyphenate LESA with a gas phase separation technique. One such technique is high-field asymmetric waveform ion mobility (FAIMS), in which ions are separated according to their different mobilities in high and low electric fields. Here, we describe the protocols for LESA FAIMS mass spectrometry of intact proteins in thin tissue sections and bacterial colonies.
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31
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Dapic I, Baljeu-Neuman L, Uwugiaren N, Kers J, Goodlett DR, Corthals GL. Proteome analysis of tissues by mass spectrometry. MASS SPECTROMETRY REVIEWS 2019; 38:403-441. [PMID: 31390493 DOI: 10.1002/mas.21598] [Citation(s) in RCA: 27] [Impact Index Per Article: 5.4] [Reference Citation Analysis] [Abstract] [Key Words] [MESH Headings] [Track Full Text] [Subscribe] [Scholar Register] [Received: 03/20/2019] [Accepted: 06/17/2019] [Indexed: 06/10/2023]
Abstract
Tissues and biofluids are important sources of information used for the detection of diseases and decisions on patient therapies. There are several accepted methods for preservation of tissues, among which the most popular are fresh-frozen and formalin-fixed paraffin embedded methods. Depending on the preservation method and the amount of sample available, various specific protocols are available for tissue processing for subsequent proteomic analysis. Protocols are tailored to answer various biological questions, and as such vary in lysis and digestion conditions, as well as duration. The existence of diverse tissue-sample protocols has led to confusion in how to choose the best protocol for a given tissue and made it difficult to compare results across sample types. Here, we summarize procedures used for tissue processing for subsequent bottom-up proteomic analysis. Furthermore, we compare protocols for their variations in the composition of lysis buffers, digestion procedures, and purification steps. For example, reports have shown that lysis buffer composition plays an important role in the profile of extracted proteins: the most common are tris(hydroxymethyl)aminomethane, radioimmunoprecipitation assay, and ammonium bicarbonate buffers. Although, trypsin is the most commonly used enzyme for proteolysis, in some protocols it is supplemented with Lys-C and/or chymotrypsin, which will often lead to an increase in proteome coverage. Data show that the selection of the lysis procedure might need to be tissue-specific to produce distinct protocols for individual tissue types. Finally, selection of the procedures is also influenced by the amount of sample available, which range from biopsies or the size of a few dozen of mm2 obtained with laser capture microdissection to much larger amounts that weight several milligrams.
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Affiliation(s)
- Irena Dapic
- International Centre for Cancer Vaccine Science, University of Gdansk, Gdansk, Poland
| | | | - Naomi Uwugiaren
- International Centre for Cancer Vaccine Science, University of Gdansk, Gdansk, Poland
| | - Jesper Kers
- Department of Pathology, Amsterdam Infection & Immunity Institute (AI&II), Amsterdam Cardiovascular Sciences (ACS), Amsterdam UMC, University of Amsterdam, Amsterdam, The Netherlands
- van 't Hoff Institute for Molecular Sciences, University of Amsterdam, Amsterdam, The Netherlands
- Ragon Institute of Massachusetts General Hospital, Massachusetts Institute of Technology and Harvard University, Cambridge, MA
| | - David R Goodlett
- International Centre for Cancer Vaccine Science, University of Gdansk, Gdansk, Poland
- University of Maryland, 20N. Pine Street, Baltimore, MD 21201
| | - Garry L Corthals
- van 't Hoff Institute for Molecular Sciences, University of Amsterdam, Amsterdam, The Netherlands
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32
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Shvartsburg AA, Andrzejewski R, Entwistle A, Giles R. Ion Mobility Spectrometry of Macromolecules with Dipole Alignment Switchable by Varying the Gas Pressure. Anal Chem 2019; 91:8176-8183. [DOI: 10.1021/acs.analchem.9b00525] [Citation(s) in RCA: 8] [Impact Index Per Article: 1.6] [Reference Citation Analysis] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Indexed: 12/12/2022]
Affiliation(s)
- Alexandre A. Shvartsburg
- Department of Chemistry, Wichita State University, 1845 Fairmount, Wichita, Kansas 67260, United States
| | - Roch Andrzejewski
- Shimadzu Research Laboratory, Wharfside, Trafford Wharf Road, Manchester M17 1GP, United Kingdom
| | - Andrew Entwistle
- Shimadzu Research Laboratory, Wharfside, Trafford Wharf Road, Manchester M17 1GP, United Kingdom
| | - Roger Giles
- Shimadzu Research Laboratory, Wharfside, Trafford Wharf Road, Manchester M17 1GP, United Kingdom
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33
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Duncan KD, Lanekoff I. Spatially Defined Surface Sampling Capillary Electrophoresis Mass Spectrometry. Anal Chem 2019; 91:7819-7827. [DOI: 10.1021/acs.analchem.9b01516] [Citation(s) in RCA: 7] [Impact Index Per Article: 1.4] [Reference Citation Analysis] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Indexed: 02/07/2023]
Affiliation(s)
- Kyle D. Duncan
- Department of Chemistry-BMC, Uppsala University, Uppsala 751 24, Sweden
| | - Ingela Lanekoff
- Department of Chemistry-BMC, Uppsala University, Uppsala 751 24, Sweden
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34
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Feider CL, Krieger A, DeHoog RJ, Eberlin LS. Ambient Ionization Mass Spectrometry: Recent Developments and Applications. Anal Chem 2019; 91:4266-4290. [PMID: 30790515 PMCID: PMC7444024 DOI: 10.1021/acs.analchem.9b00807] [Citation(s) in RCA: 260] [Impact Index Per Article: 52.0] [Reference Citation Analysis] [MESH Headings] [Grants] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Indexed: 12/12/2022]
Affiliation(s)
- Clara L. Feider
- Department of Chemistry, The University of Texas at Austin, Austin, Texas 78712, United States
| | - Anna Krieger
- Department of Chemistry, The University of Texas at Austin, Austin, Texas 78712, United States
| | - Rachel J. DeHoog
- Department of Chemistry, The University of Texas at Austin, Austin, Texas 78712, United States
| | - Livia S. Eberlin
- Department of Chemistry, The University of Texas at Austin, Austin, Texas 78712, United States
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35
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Kocurek KI, May RC, Cooper HJ. Application of High-Field Asymmetric Waveform Ion Mobility Separation to LESA Mass Spectrometry of Bacteria. Anal Chem 2019; 91:4755-4761. [DOI: 10.1021/acs.analchem.9b00307] [Citation(s) in RCA: 8] [Impact Index Per Article: 1.6] [Reference Citation Analysis] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Indexed: 11/30/2022]
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36
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Winter DL, Wilkins MR, Donald WA. Differential Ion Mobility–Mass Spectrometry for Detailed Analysis of the Proteome. Trends Biotechnol 2019; 37:198-213. [DOI: 10.1016/j.tibtech.2018.07.018] [Citation(s) in RCA: 30] [Impact Index Per Article: 6.0] [Reference Citation Analysis] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Received: 05/30/2018] [Revised: 07/27/2018] [Accepted: 07/30/2018] [Indexed: 10/28/2022]
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37
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Nagy G, Veličković D, Chu RK, Carrell AA, Weston DJ, Ibrahim YM, Anderton CR, Smith RD. Towards resolving the spatial metabolome with unambiguous molecular annotations in complex biological systems by coupling mass spectrometry imaging with structures for lossless ion manipulations. Chem Commun (Camb) 2019; 55:306-309. [PMID: 30534702 PMCID: PMC6537888 DOI: 10.1039/c8cc07482h] [Citation(s) in RCA: 21] [Impact Index Per Article: 4.2] [Reference Citation Analysis] [Abstract] [Grants] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Indexed: 12/15/2022]
Abstract
We demonstrate the coupling of liquid extraction surface analysis (LESA) to structures for lossless ion manipulations in conjunction with serpentine ultralong path with extending routing (SLIM SUPER) ion mobility-mass spectrometry (IM-MS) for the unambiguous annotation of important isomeric glycoforms in carbon-fixing communities.
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Affiliation(s)
- Gabe Nagy
- Biological Sciences Division, Pacific Northwest National Laboratory, Richland, WA 99352, USA.
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38
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Neagu AN. Proteome Imaging: From Classic to Modern Mass Spectrometry-Based Molecular Histology. ADVANCES IN EXPERIMENTAL MEDICINE AND BIOLOGY 2019; 1140:55-98. [PMID: 31347042 DOI: 10.1007/978-3-030-15950-4_4] [Citation(s) in RCA: 4] [Impact Index Per Article: 0.8] [Reference Citation Analysis] [Abstract] [Key Words] [Track Full Text] [Subscribe] [Scholar Register] [Indexed: 12/19/2022]
Abstract
In order to overcome the limitations of classic imaging in Histology during the actually era of multiomics, the multi-color "molecular microscope" by its emerging "molecular pictures" offers quantitative and spatial information about thousands of molecular profiles without labeling of potential targets. Healthy and diseased human tissues, as well as those of diverse invertebrate and vertebrate animal models, including genetically engineered species and cultured cells, can be easily analyzed by histology-directed MALDI imaging mass spectrometry. The aims of this review are to discuss a range of proteomic information emerging from MALDI mass spectrometry imaging comparative to classic histology, histochemistry and immunohistochemistry, with applications in biology and medicine, concerning the detection and distribution of structural proteins and biological active molecules, such as antimicrobial peptides and proteins, allergens, neurotransmitters and hormones, enzymes, growth factors, toxins and others. The molecular imaging is very well suited for discovery and validation of candidate protein biomarkers in neuroproteomics, oncoproteomics, aging and age-related diseases, parasitoproteomics, forensic, and ecotoxicology. Additionally, in situ proteome imaging may help to elucidate the physiological and pathological mechanisms involved in developmental biology, reproductive research, amyloidogenesis, tumorigenesis, wound healing, neural network regeneration, matrix mineralization, apoptosis and oxidative stress, pain tolerance, cell cycle and transformation under oncogenic stress, tumor heterogeneity, behavior and aggressiveness, drugs bioaccumulation and biotransformation, organism's reaction against environmental penetrating xenobiotics, immune signaling, assessment of integrity and functionality of tissue barriers, behavioral biology, and molecular origins of diseases. MALDI MSI is certainly a valuable tool for personalized medicine and "Eco-Evo-Devo" integrative biology in the current context of global environmental challenges.
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Affiliation(s)
- Anca-Narcisa Neagu
- Laboratory of Animal Histology, Faculty of Biology, "Alexandru Ioan Cuza" University of Iasi, Iasi, Romania.
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39
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Vaysse PM, Heeren RMA, Porta T, Balluff B. Mass spectrometry imaging for clinical research - latest developments, applications, and current limitations. Analyst 2018. [PMID: 28642940 DOI: 10.1039/c7an00565b] [Citation(s) in RCA: 136] [Impact Index Per Article: 22.7] [Reference Citation Analysis] [Abstract] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Indexed: 12/11/2022]
Abstract
Mass spectrometry is being used in many clinical research areas ranging from toxicology to personalized medicine. Of all the mass spectrometry techniques, mass spectrometry imaging (MSI), in particular, has continuously grown towards clinical acceptance. Significant technological and methodological improvements have contributed to enhance the performance of MSI recently, pushing the limits of throughput, spatial resolution, and sensitivity. This has stimulated the spread of MSI usage across various biomedical research areas such as oncology, neurological disorders, cardiology, and rheumatology, just to name a few. After highlighting the latest major developments and applications touching all aspects of translational research (i.e. from early pre-clinical to clinical research), we will discuss the present challenges in translational research performed with MSI: data management and analysis, molecular coverage and identification capabilities, and finally, reproducibility across multiple research centers, which is the largest remaining obstacle in moving MSI towards clinical routine.
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Affiliation(s)
- Pierre-Maxence Vaysse
- Maastricht MultiModal Molecular Imaging (M4I) institute, Division of Imaging Mass Spectrometry, Maastricht University, Universiteitssingel 50, 6229 ER, Maastricht, The Netherlands.
| | - Ron M A Heeren
- Maastricht MultiModal Molecular Imaging (M4I) institute, Division of Imaging Mass Spectrometry, Maastricht University, Universiteitssingel 50, 6229 ER, Maastricht, The Netherlands.
| | - Tiffany Porta
- Maastricht MultiModal Molecular Imaging (M4I) institute, Division of Imaging Mass Spectrometry, Maastricht University, Universiteitssingel 50, 6229 ER, Maastricht, The Netherlands.
| | - Benjamin Balluff
- Maastricht MultiModal Molecular Imaging (M4I) institute, Division of Imaging Mass Spectrometry, Maastricht University, Universiteitssingel 50, 6229 ER, Maastricht, The Netherlands.
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40
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Towers MW, Karancsi T, Jones EA, Pringle SD, Claude E. Optimised Desorption Electrospray Ionisation Mass Spectrometry Imaging (DESI-MSI) for the Analysis of Proteins/Peptides Directly from Tissue Sections on a Travelling Wave Ion Mobility Q-ToF. JOURNAL OF THE AMERICAN SOCIETY FOR MASS SPECTROMETRY 2018; 29:2456-2466. [PMID: 30168053 PMCID: PMC6276080 DOI: 10.1007/s13361-018-2049-0] [Citation(s) in RCA: 70] [Impact Index Per Article: 11.7] [Reference Citation Analysis] [Abstract] [Key Words] [MESH Headings] [Track Full Text] [Subscribe] [Scholar Register] [Received: 03/23/2018] [Revised: 07/20/2018] [Accepted: 08/03/2018] [Indexed: 05/04/2023]
Abstract
Desorption electrospray ionisation mass spectrometry imaging (DESI-MSI) is typically known for the ionisation of small molecules such as lipids and metabolites, in singly charged form. Here we present a method that allows the direct detection of proteins and peptides in multiply charged forms directly from tissue sections by DESI. Utilising a heated mass spectrometer inlet capillary, combined with ion mobility separation (IMS), the conditions with regard to solvent composition, nebulising gas flow, and solvent flow rate have been explored and optimised. Without the use of ion mobility separation prior to mass spectrometry analysis, only the most abundant charge series were observed. In addition to the dominant haemoglobin subunit(s) related trend line in the m/z vs drift time (DT) 2D plot, trend lines were found relating to background solvent peaks, residual lipids and, more importantly, small proteins/large peptides of lower abundance. These small proteins/peptides were observed with charge states from 1+ to 12+, the majority of which could only be resolved from the background when using IMS. By extracting charge series from the 2D m/z vs DT plot, a number of proteins could be tentatively assigned by accurate mass. Tissue images were acquired with a pixel size of 150 μm showing a marked improvement in protein image resolution compared to other liquid-based ambient imaging techniques such as liquid extraction surface analysis (LESA) and continuous-flow liquid microjunction surface sampling probe (LMJ-SSP) imaging. Graphical Abstract ᅟ.
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Affiliation(s)
- Mark W Towers
- Waters Corporation, Stamford Avenue, Altricham Road, Wilmslow, SK9 4AX, UK.
| | - Tamas Karancsi
- Waters Research Centre, Záhony utca., C ép., 1. Em., Budapest, 1031, Hungary
| | - Emrys A Jones
- Waters Corporation, Stamford Avenue, Altricham Road, Wilmslow, SK9 4AX, UK
| | - Steven D Pringle
- Waters Corporation, Stamford Avenue, Altricham Road, Wilmslow, SK9 4AX, UK
| | - Emmanuelle Claude
- Waters Corporation, Stamford Avenue, Altricham Road, Wilmslow, SK9 4AX, UK
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41
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Lopez-Clavijo AF, Griffiths RL, Goodwin RJA, Cooper HJ. Liquid Extraction Surface Analysis (LESA) Electron-Induced Dissociation and Collision-Induced Dissociation Mass Spectrometry of Small Molecule Drug Compounds. JOURNAL OF THE AMERICAN SOCIETY FOR MASS SPECTROMETRY 2018; 29:2218-2226. [PMID: 30151679 DOI: 10.1007/s13361-018-2042-7] [Citation(s) in RCA: 10] [Impact Index Per Article: 1.7] [Reference Citation Analysis] [Abstract] [Key Words] [MESH Headings] [Track Full Text] [Subscribe] [Scholar Register] [Received: 05/25/2018] [Revised: 07/26/2018] [Accepted: 07/27/2018] [Indexed: 06/08/2023]
Abstract
Here, we present liquid extraction surface analysis (LESA) coupled with electron-induced dissociation (EID) mass spectrometry in a Fourier-transform ion cyclotron resonance mass spectrometer for the analysis of small organic pharmaceutical compounds directly from dosed tissue. First, the direct infusion electrospray ionisation EID and collision-induced dissociation (CID) behaviour of erlotinib, moxifloxacin, clozapine and olanzapine standards were compared. EID mass spectra were also compared with experimental or reference electron impact ionisation mass spectra. The results show that (with the exception of erlotinib) EID and CID result in complementary fragment ions. Subsequently, we performed LESA EID MS/MS and LESA CID MS/MS on singly charged ions of moxifloxacin and erlotinib extracted from a thin tissue section of rat kidney from a cassette-dosed animal. Both techniques provided structural information, with the majority of peaks observed for the drug standards also observed for the tissue-extracted species. Overall, these results demonstrate the feasibility of LESA EID MS/MS of drug compounds from dosed tissue and extend the number of molecular structures for which EID behaviour has been determined. Graphical Abstract ᅟ.
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Affiliation(s)
| | - Rian L Griffiths
- School of Biosciences, University of Birmingham, Birmingham, B15 2TT, UK
| | - Richard J A Goodwin
- Pathology, Drug Safety & Metabolism, IMED Biotech Unit, AstraZeneca, Darwin Building, Cambridge Science Park, Milton Road, Cambridge, CB4 0WG, UK
| | - Helen J Cooper
- School of Biosciences, University of Birmingham, Birmingham, B15 2TT, UK.
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42
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Griffiths RL, Simmonds AL, Swales JG, Goodwin RJA, Cooper HJ. LESA MS Imaging of Heat-Preserved and Frozen Tissue: Benefits of Multistep Static FAIMS. Anal Chem 2018; 90:13306-13314. [DOI: 10.1021/acs.analchem.8b02739] [Citation(s) in RCA: 18] [Impact Index Per Article: 3.0] [Reference Citation Analysis] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Indexed: 01/07/2023]
Affiliation(s)
- Rian L. Griffiths
- School of Biosciences, University of Birmingham, Edgbaston B15 2TT, U.K
| | - Anna L. Simmonds
- School of Biosciences, University of Birmingham, Edgbaston B15 2TT, U.K
| | - John G. Swales
- Pathology, Drug Safety & Metabolism, IMED Biotech Unit, AstraZeneca, Darwin Building, Cambridge Science Park, Milton Road, Cambridge CB4 0WG, U.K
| | - Richard J. A. Goodwin
- Pathology, Drug Safety & Metabolism, IMED Biotech Unit, AstraZeneca, Darwin Building, Cambridge Science Park, Milton Road, Cambridge CB4 0WG, U.K
| | - Helen J. Cooper
- School of Biosciences, University of Birmingham, Edgbaston B15 2TT, U.K
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43
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Kocurek KI, Griffiths RL, Cooper HJ. Ambient ionisation mass spectrometry for in situ analysis of intact proteins. JOURNAL OF MASS SPECTROMETRY : JMS 2018; 53:565-578. [PMID: 29607564 PMCID: PMC6001466 DOI: 10.1002/jms.4087] [Citation(s) in RCA: 9] [Impact Index Per Article: 1.5] [Reference Citation Analysis] [Abstract] [Key Words] [MESH Headings] [Track Full Text] [Subscribe] [Scholar Register] [Received: 02/23/2018] [Revised: 03/21/2018] [Accepted: 03/22/2018] [Indexed: 05/05/2023]
Abstract
Ambient surface mass spectrometry is an emerging field which shows great promise for the analysis of biomolecules directly from their biological substrate. In this article, we describe ambient ionisation mass spectrometry techniques for the in situ analysis of intact proteins. As a broad approach, the analysis of intact proteins offers unique advantages for the determination of primary sequence variations and posttranslational modifications, as well as interrogation of tertiary and quaternary structure and protein-protein/ligand interactions. In situ analysis of intact proteins offers the potential to couple these advantages with information relating to their biological environment, for example, their spatial distributions within healthy and diseased tissues. Here, we describe the techniques most commonly applied to in situ protein analysis (liquid extraction surface analysis, continuous flow liquid microjunction surface sampling, nano desorption electrospray ionisation, and desorption electrospray ionisation), their advantages, and limitations and describe their applications to date. We also discuss the incorporation of ion mobility spectrometry techniques (high field asymmetric waveform ion mobility spectrometry and travelling wave ion mobility spectrometry) into ambient workflows. Finally, future directions for the field are discussed.
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Affiliation(s)
- Klaudia I. Kocurek
- School of BiosciencesUniversity of BirminghamEdgbastonBirminghamB15 2TTUK
| | - Rian L. Griffiths
- School of BiosciencesUniversity of BirminghamEdgbastonBirminghamB15 2TTUK
| | - Helen J. Cooper
- School of BiosciencesUniversity of BirminghamEdgbastonBirminghamB15 2TTUK
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44
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Garza KY, Feider CL, Klein DR, Rosenberg JA, Brodbelt JS, Eberlin LS. Desorption Electrospray Ionization Mass Spectrometry Imaging of Proteins Directly from Biological Tissue Sections. Anal Chem 2018; 90:7785-7789. [PMID: 29800516 DOI: 10.1021/acs.analchem.8b00967] [Citation(s) in RCA: 88] [Impact Index Per Article: 14.7] [Reference Citation Analysis] [Abstract] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Indexed: 01/04/2023]
Abstract
Analysis of large biomolecules including proteins has proven challenging using ambient ionization mass spectrometry imaging techniques. Here, we have successfully optimized desorption electrospray ionization mass spectrometry (DESI-MS) to detect intact proteins directly from tissue sections and further integrated DESI-MS to a high field asymmetric waveform ion mobility (FAIMS) device for protein imaging. Optimized DESI-FAIMS-MS parameters were used to image mouse kidney, mouse brain, and human ovarian and breast tissue samples, allowing detection of 11, 16, 14, and 16 proteoforms, respectively. Identification of protein species detected by DESI-MS was performed on-tissue by top-down ultraviolet photodissociation (UVPD) and collision induced dissociation (CID) as well as using tissue extracts by bottom-up CID and top-down UVPD. Our results demonstrate that DESI-MS imaging is suitable for the analysis of the distribution of proteins within biological tissue sections.
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Affiliation(s)
- Kyana Y Garza
- Department of Chemistry , The University of Texas at Austin , Austin , Texas 78712 , United States
| | - Clara L Feider
- Department of Chemistry , The University of Texas at Austin , Austin , Texas 78712 , United States
| | - Dustin R Klein
- Department of Chemistry , The University of Texas at Austin , Austin , Texas 78712 , United States
| | - Jake A Rosenberg
- Department of Chemistry , The University of Texas at Austin , Austin , Texas 78712 , United States
| | - Jennifer S Brodbelt
- Department of Chemistry , The University of Texas at Austin , Austin , Texas 78712 , United States
| | - Livia S Eberlin
- Department of Chemistry , The University of Texas at Austin , Austin , Texas 78712 , United States
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45
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Rosting C, Yu J, Cooper HJ. High Field Asymmetric Waveform Ion Mobility Spectrometry in Nontargeted Bottom-up Proteomics of Dried Blood Spots. J Proteome Res 2018; 17:1997-2004. [DOI: 10.1021/acs.jproteome.7b00746] [Citation(s) in RCA: 19] [Impact Index Per Article: 3.2] [Reference Citation Analysis] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Indexed: 02/07/2023]
Affiliation(s)
| | - Jinglei Yu
- School of Biosciences, University of Birmingham, Birmingham B15 2TT, U.K
| | - Helen J. Cooper
- School of Biosciences, University of Birmingham, Birmingham B15 2TT, U.K
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46
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Meurs J, Alexander MR, Levkin PA, Widmaier S, Bunch J, Barrett DA, Kim DH. Improved Extraction Repeatability and Spectral Reproducibility for Liquid Extraction Surface Analysis–Mass Spectrometry Using Superhydrophobic–Superhydrophilic Patterning. Anal Chem 2018; 90:6001-6005. [DOI: 10.1021/acs.analchem.8b00973] [Citation(s) in RCA: 11] [Impact Index Per Article: 1.8] [Reference Citation Analysis] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Indexed: 01/13/2023]
Affiliation(s)
- Joris Meurs
- Advanced Materials and Healthcare Technology Division, School of Pharmacy, University of Nottingham, University Park, Nottingham, NG7 2RD, United Kingdom
| | - Morgan R. Alexander
- Advanced Materials and Healthcare Technology Division, School of Pharmacy, University of Nottingham, University Park, Nottingham, NG7 2RD, United Kingdom
| | - Pavel A. Levkin
- Institute of Toxicology and Genetics, Karlsruhe Institute of Technology (KIT), Hermann-von-Helmholtz Platz 1, Eggenstein-Leopoldshafen, 76344, Germany
- Institute of Organic Chemistry, Karlsruhe Institute of Technology (KIT), Karlsruhe, 76131, Germany
| | - Simon Widmaier
- Institute of Toxicology and Genetics, Karlsruhe Institute of Technology (KIT), Hermann-von-Helmholtz Platz 1, Eggenstein-Leopoldshafen, 76344, Germany
| | - Josephine Bunch
- National Centre of Excellence in Mass Spectrometry Imaging, National Physical Laboratory, Hampton Road, Teddington, Middlesex TW11 0LW, United Kingdom
| | - David A. Barrett
- Advanced Materials and Healthcare Technology Division, School of Pharmacy, University of Nottingham, University Park, Nottingham, NG7 2RD, United Kingdom
| | - Dong-Hyun Kim
- Advanced Materials and Healthcare Technology Division, School of Pharmacy, University of Nottingham, University Park, Nottingham, NG7 2RD, United Kingdom
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47
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Ambient surface mass spectrometry–ion mobility spectrometry of intact proteins. Curr Opin Chem Biol 2018; 42:67-75. [DOI: 10.1016/j.cbpa.2017.11.002] [Citation(s) in RCA: 8] [Impact Index Per Article: 1.3] [Reference Citation Analysis] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Received: 08/17/2017] [Revised: 10/31/2017] [Accepted: 11/02/2017] [Indexed: 11/18/2022]
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48
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Sans M, Feider CL, Eberlin LS. Advances in mass spectrometry imaging coupled to ion mobility spectrometry for enhanced imaging of biological tissues. Curr Opin Chem Biol 2018; 42:138-146. [PMID: 29275246 PMCID: PMC5828985 DOI: 10.1016/j.cbpa.2017.12.005] [Citation(s) in RCA: 75] [Impact Index Per Article: 12.5] [Reference Citation Analysis] [Abstract] [MESH Headings] [Grants] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Received: 09/04/2017] [Revised: 12/04/2017] [Accepted: 12/11/2017] [Indexed: 11/20/2022]
Abstract
Tissues present complex biochemical and morphological composition associated with their various cell types and physiological functions. Mass spectrometry (MS) imaging technologies are powerful tools to investigate the molecular information from biological tissue samples and visualize their complex spatial distributions. Coupling of gas-phase ion mobility spectrometry (IMS) technologies to MS imaging has been increasingly explored to improve performance for biological tissue imaging. This approach allows improved detection of low abundance ions and separation of isobaric molecular species, thus resulting in more accurate determination of the spatial distribution of molecular ions. In this review, we highlight recent advances in the field focusing on promising applications of these technologies for metabolite, lipid and protein tissue imaging.
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Affiliation(s)
- Marta Sans
- Department of Chemistry, The University of Texas at Austin, Austin, TX 78712, United States
| | - Clara L Feider
- Department of Chemistry, The University of Texas at Austin, Austin, TX 78712, United States
| | - Livia S Eberlin
- Department of Chemistry, The University of Texas at Austin, Austin, TX 78712, United States.
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49
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Rae Buchberger A, DeLaney K, Johnson J, Li L. Mass Spectrometry Imaging: A Review of Emerging Advancements and Future Insights. Anal Chem 2018; 90:240-265. [PMID: 29155564 PMCID: PMC5959842 DOI: 10.1021/acs.analchem.7b04733] [Citation(s) in RCA: 541] [Impact Index Per Article: 90.2] [Reference Citation Analysis] [MESH Headings] [Grants] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Indexed: 02/07/2023]
Affiliation(s)
- Amanda Rae Buchberger
- Department of Chemistry, University of Wisconsin-Madison, 1101 University Avenue, Madison, Wisconsin 53706, United States
| | - Kellen DeLaney
- Department of Chemistry, University of Wisconsin-Madison, 1101 University Avenue, Madison, Wisconsin 53706, United States
| | - Jillian Johnson
- School of Pharmacy, University of Wisconsin-Madison, 777 Highland Avenue, Madison, Wisconsin 53705, United States
| | - Lingjun Li
- Department of Chemistry, University of Wisconsin-Madison, 1101 University Avenue, Madison, Wisconsin 53706, United States
- School of Pharmacy, University of Wisconsin-Madison, 777 Highland Avenue, Madison, Wisconsin 53705, United States
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50
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Microscale differential ion mobility spectrometry for field deployable chemical analysis. Trends Analyt Chem 2017. [DOI: 10.1016/j.trac.2017.10.011] [Citation(s) in RCA: 26] [Impact Index Per Article: 3.7] [Reference Citation Analysis] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Indexed: 11/20/2022]
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