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      Toward an Optimized Workflow for Middle-Down Proteomics


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          Mass spectrometry (MS)-based proteomics workflows can crudely be classified into two distinct regimes, targeting either relatively small peptides (i.e., 0.7 kDa < M w < 3.0 kDa) or small to medium sized intact proteins (i.e., 10 kDa < M w < 30 kDa), respectively, termed bottom-up and top-down proteomics. Recently, a niche has started to be explored covering the analysis of middle-range peptides (i.e., 3.0 kDa < M w < 10 kDa), aptly termed middle-down proteomics. Although middle-down proteomics can follow, in principle, a modular workflow similar to that of bottom-up proteomics, we hypothesized that each of these modules would benefit from targeted optimization to improve its overall performance in the analysis of middle-range sized peptides. Hence, to generate middle-range sized peptides from cellular lysates, we explored the use of the proteases Asp-N and Glu-C and a nonenzymatic acid induced cleavage. To increase the depth of the proteome, a strong cation exchange (SCX) separation, carefully tuned to improve the separation of longer peptides, combined with reversed phase-liquid chromatography (RP-LC) using columns packed with material possessing a larger pore size, was used. Finally, after evaluating the combination of potentially beneficial MS settings, we also assessed the peptide fragmentation techniques, including higher-energy collision dissociation (HCD), electron-transfer dissociation (ETD), and electron-transfer combined with higher-energy collision dissociation (EThcD), for characterization of middle-range sized peptides. These combined improvements clearly improve the detection and sequence coverage of middle-range peptides and should guide researchers to explore further how middle-down proteomics may lead to an improved proteome coverage, beneficial for, among other things, the enhanced analysis of (co-occurring) post-translational modifications.

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          Most cited references 48

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          Peptide and protein sequence analysis by electron transfer dissociation mass spectrometry.

          Peptide sequence analysis using a combination of gas-phase ion/ion chemistry and tandem mass spectrometry (MS/MS) is demonstrated. Singly charged anthracene anions transfer an electron to multiply protonated peptides in a radio frequency quadrupole linear ion trap (QLT) and induce fragmentation of the peptide backbone along pathways that are analogous to those observed in electron capture dissociation. Modifications to the QLT that enable this ion/ion chemistry are presented, and automated acquisition of high-quality, single-scan electron transfer dissociation MS/MS spectra of phosphopeptides separated by nanoflow HPLC is described.
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            Combination of FASP and StageTip-based fractionation allows in-depth analysis of the hippocampal membrane proteome.

            Membrane proteomics is challenging because the desirable strong detergents are incompatible with downstream analysis. Recently, we demonstrated efficient removal of SDS by the filter aided sample preparation method (FASP). Here we combine FASP with our previously described small-scale membrane enrichment protocol. Analysis of a single mouse hippocampus enables identification of more than 1000 membrane proteins in a single LC-MS/MS run without protein or peptide prefractionation. To extend proteome coverage, we developed a simple anion exchange fractionation method in a StageTip format. When separating peptides into six fractions, a duplicate analysis resulted in identification of 4206 proteins of which 64% were membrane proteins. This data set covers 83% of glutamate and GABA receptor subunits identified in hippocampus in the Allen Brain Atlas and adds further isoforms. The combined method provides a streamlined protocol for rapid and sensitive membrane proteome mapping. We also provide a generic protocol for combining FASP with StageTip-based ion exchange fractionation, which is generally applicable to proteome analysis.
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              Mapping Intact Protein Isoforms in Discovery Mode Using Top Down Proteomics

              A full description of the human proteome relies on the challenging task of detecting mature and changing forms of protein molecules in the body. Large scale proteome analysis 1 has routinely involved digesting intact proteins followed by inferred protein identification using mass spectrometry (MS) 2 . This “bottom up” process affords a high number of identifications (not always unique to a single gene). However, complications arise from incomplete or ambiguous 2 characterization of alternative splice forms, diverse modifications (e.g., acetylation and methylation), and endogenous protein cleavages, especially when combinations of these create complex patterns of intact protein isoforms and species 3 . “Top down” interrogation of whole proteins can overcome these problems for individual proteins 4,5 , but has not been achieved on a proteome scale due to the lack of intact protein fractionation methods that are well integrated with tandem MS. Here we show, using a new four dimensional (4D) separation system, identification of 1,043 gene products from human cells that are dispersed into >3,000 protein species created by post-translational modification, RNA splicing, and proteolysis. The overall system produced >20-fold increases in both separation power and proteome coverage, enabling the identification of proteins up to 105 kilodaltons and those with up to 11 transmembrane helices. Many previously undetected isoforms of endogenous human proteins were mapped, including changes in multiply-modified species in response to accelerated cellular aging (senescence) induced by DNA damage. Integrated with the latest version of the Swiss-Prot database 6 , the data provide precise correlations to individual genes and proof-of-concept for large scale interrogation of whole protein molecules. The technology promises to improve the link between proteomics data and complex phenotypes in basic biology and disease research 7 .

                Author and article information

                Anal Chem
                Anal. Chem
                Analytical Chemistry
                American Chemical Society
                24 February 2017
                21 March 2017
                : 89
                : 6
                : 3318-3325
                []Biomolecular Mass Spectrometry and Proteomics Group, Bijvoet Center for Biomolecular Research, Utrecht University , Padualaan 8, 3584 CH Utrecht, The Netherlands
                []Netherlands Proteomics Center , Padualaan 8, 3584 CH Utrecht, The Netherlands
                [§ ]Departments of Chemistry and Biochemistry, University of Oxford , New Biochemistry Building, South Parks Road, Oxford, OX1 3QU Oxfordshire, United Kingdom
                Author notes
                [* ]E-mail: a.j.r.heck@ 123456uu.nl (A.J.R.H.).
                Copyright © 2017 American Chemical Society

                This is an open access article published under a Creative Commons Non-Commercial No Derivative Works (CC-BY-NC-ND) Attribution License, which permits copying and redistribution of the article, and creation of adaptations, all for non-commercial purposes.

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                Analytical chemistry


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