Evaluation of the application of sodium deoxycholate to proteomic analysis of rat hippocampal plasma membrane

Detergents have been widely used for the solubilization of membrane proteins and the improvement of their digestion. In this paper, we have evaluated the application of sodium deoxycholate (SDC) to the solubilization and digestion of rat hippocampal plasma membrane (PM) proteins. For in-solution digestion, rat hippocampal PM fraction from sucrose-density gradient centrifugation was solubilized by boiling in 1.0% SDC, and directly digested without dilution. During the in-gel digestion of the hippocampal PM proteins separated by SDS-PAGE, 0.1% SDC was added. Before analysis of peptide mixture by liquid chromatography and electrospray mass spectrometry, SDC in the tryptic digests was removed by centrifugation following acidification. Use of 1.0% SDC in solubilization and in-solution digestion of rat PM proteins had led to 77 PM or membrane-associated proteins identified, a more than 2-fold increase over that by use of SDS. The addition of 0.1% SDC to the in-gel digestion of SDS-PAGE-resolved membrane proteins remarkably enhanced the coverage of tryptic peptides and the number of hydrophobic membrane proteins identified. Being a cheaper and more tractable acid-insoluble detergent, SDC could be used at higher concentration in the solubilization and tryptic digestion of proteins including PM proteins with the purpose of enhancing the protein solubility and at the same time making no interference with trypsin activity and subsequent analyses.     

Sodium-deoxycholate-assisted tryptic digestion and identification of proteolytically resistant proteins

Identification of proteolytically resistant proteins with compact molecular structure and/or poor water solubility is a challenge in current proteomic study. In this study, sodium deoxycholate (SDC)-assisted tryptic digestion and identification of proteolytically resistant myoglobin and integral membrane proteins were systematically investigated. When the effect of SDC up to 10% on trypsin activity was investigated, little decrease in the trypsin activity was observed in 1% SDC solution, 2-5% SDC decreased the enzyme activity only by about 13.6%, and even in the presence of 10% SDC trypsin still retained 77.4% of its activity. Matrix-assisted laser desorption ionization time of flight mass spectrometry analysis showed that SDC could be removed from sample solution with acid treatment followed by centrifugation, and the remaining SDC, if any, had little effect on mass spectrometry analysis with regard to the number and signal/noise ratio of ions in the mass spectra. Compared with urea and methanol, two other commonly used additives in addition to SDS in proteomic analysis, SDC improved more efficiently the denaturation, solubilization, and tryptic digestion of proteins, particularly proteolytically resistant myoglobin and integral membrane proteins, thereby enhancing the efficiency of their identification with regard to the number of identified proteins and unique peptides and the sequence coverage of matched proteins.     

An in-gel digestion procedure that facilitates the identification of highly hydrophobic proteins by electrospray ionization-mass spectrometry analysis

A procedure is described for in-gel tryptic digestion of proteins that allows the direct analysis of eluted peptides in electrospray ionization (ESI) mass spectrometers without the need of a postdigestion desalting step. It is based on the following principles: (a) a thorough desalting of the protein in-gel before digestion that takes advantage of the excellent properties of acrylamide polymers for size exclusion separations, (b) exploiting the activity of trypsin in water, in the absence of inorganic buffers, and (c) a procedure for peptide extraction using solvents of proven efficacy with highly hydrophobic peptides. Quality of spectra and sequence coverage are equivalent to those obtained after digestion in ammonium bicarbonate for hydrophilic proteins detected with Coomassie blue, mass spectrometry-compatible silver or imidazole-zinc but are significantly superior for highly hydrophobic proteins, such as membrane proteins with several transmembrane domains. ATPase subunit 9 (GRAVY 1.446) is a membrane protein channel, lipid-binding protein for which both the conventional in-gel digestion protocol and in solution digestion failed. It was identified with very high sequence coverage. Sample handling after digestion is notably simplified as peptides are directly loaded into the ESI source without postdigestion processing, increasing the chances for the identification of hydrophobic peptides.     

Sodium Laurate,a Novel Protease- and Mass Spectrometry-Compatible Detergent for Mass Spectrometry-Based Membrane Proteomics

The hydrophobic nature of most membrane proteins severely complicates their extraction, proteolysis and identification. Although detergents can be used to enhance the solubility of the membrane proteins, it is often difficult for a detergent not only to have a strong ability to extract membrane proteins, but also to be compatible with the subsequent proteolysis and mass spectrometric analysis. In this study, we made evaluation on a novel application of sodium laurate (SL) to the shotgun analysis of membrane proteomes. SL was found not only to lyse the membranes and solubilize membrane proteins as efficiently as SDS, but also to be well compatible with trypsin and chymotrypsin. Furthermore, SL could be efficiently removed by phase transfer method from samples after acidification, thus ensuring not to interfere with the subsequent CapLC-MS/MS analysis of the proteolytic peptides of proteins. When SL was applied to assist the digestion and identification of a standard protein mixture containing bacteriorhodoposin and the proteins in rat liver plasma membrane-enriched fractions, it was found that, compared with other two representative enzyme- and MS-compatible detergents RapiGest SF (RGS) and sodium deoxycholate (SDC), SL exhibited obvious superiority in the identification of membrane proteins particularly those with high hydrophobicity and/or multiple transmembrane domains.     

Unbiased Quantitation of Escherichia coli Membrane Proteome Using Phase Transfer Surfactants

We developed a sample preparation protocol for rapid and unbiased analysis of the membrane proteome using an alimentary canal-mimicking system in which proteases are activated in the presence of bile salts. In this rapid and unbiased protocol, immobilized trypsin is used in the presence of deoxycholate and lauroylsarcosine to increase digestion efficiency as well as to increase the solubility of the membrane proteins. Using 22.5 μg of Escherichia coli whole cell lysate, we quantitatively demonstrated that membrane proteins were extracted and digested at the same level as soluble proteins without any solubility-related bias. The recovery of membrane proteins was independent of the number of transmembrane domains per protein. In the analysis of the membrane-enriched fraction from 22.5 μg of E. coli cell lysate, the abundance distribution of the membrane proteins was in agreement with that of the membrane protein-coding genes when this protocol, coupled with strong cation exchange prefractionation prior to nano-LC-MS/MS analysis, was used. Because this protocol allows unbiased sample preparation, protein abundance estimation based on the number of observed peptides per protein was applied to both soluble and membrane proteins simultaneously, and the copy numbers per cell for 1,453 E. coli proteins, including 545 membrane proteins, were successfully obtained. Finally, this protocol was applied to quantitative analysis of guanosine tetra- and pentaphosphate-dependent signaling in E. coli wild-type and relA knock-out strains.Despite the importance of cell surface biology, the conventional shotgun proteomics strategy generally underrepresents the membrane proteome because of inadequate solubilization and protease digestion (1, 2). The ageless gel strategy, consisting of SDS-PAGE followed by in-gel digestion, can partially solve this problem (3–5), but the recovery from in-gel digestion is generally lower than that from in-solution digestion, and this approach is far from suitable for a rapid, simple, and high throughput automated system. Numerous approaches have been reported to overcome the difficulties in membrane proteome analysis, such as the use of surfactants (2, 6–11), organic solvents (6, 7, 12–15), or chaotropic reagents (2, 6, 16). Acid-labile surfactants, such as RapiGest SF, are among the most promising additives to enhance protein solubilization without interfering with LC-MS performance (6, 10, 17–19). However, the cleavage step at acidic pH causes loss of hydrophobic peptides because of coprecipitation with the hydrophobic part of RapiGest SF (20). Recently, we developed a new protocol to dissolve and digest membrane proteins with the aid of a removable phase transfer surfactant (PTS),1 such as sodium deoxycholate (SDC) (20). The solubility of membrane proteins with SDC was comparable to that with sodium dodecyl sulfate. In addition, the activity of trypsin was enhanced ∼5-fold in the presence of 1% SDC because this rapid PTS method mimics conditions in the alimentary canal in which bile salts such as cholate and deoxycholate are secreted together with trypsin. After tryptic digestion, SDC is removed prior to LC-MS/MS analysis by adding an organic solvent followed by pH-induced transfer of the surfactant to the organic phase, whereas tryptic peptides remain in the aqueous phase. This protocol offers a significant improvement in identifying membrane proteins by increasing the recovery of hydrophobic tryptic peptides compared with the protocols using urea and RapiGest SF.The goal of this study is to establish a membrane proteomics method that is unbiased with respect to protein solubility, hydrophobicity, and protein abundance; i.e. membrane proteins can be as efficiently extracted and digested as soluble proteins. So far, to our knowledge, little information about the recovery of the membrane proteome has been reported. Instead, the number of identified membrane proteins or the content of membrane proteins identified in the membrane-enriched fraction has been used as an indicator of the efficiency of procedures for membrane proteome analysis (4, 5, 21–23). However, these parameters usually depend on the experimental conditions, including the sample preparation procedure and LC-MS instrument used. Therefore, it is difficult to compare data obtained with these protocols except in the case of direct comparison. Furthermore, there has been no report quantitatively comparing the recovery of membrane proteome with that of soluble proteins.In this study, we used a modified version of our PTS protocol with immobilized trypsin columns to reduce the digestion time and evaluated its suitability for unbiased quantitation of the membrane proteome. In addition, we applied this protocol to estimate the copy numbers per cell of 1,453 proteins, including 545 membrane proteins, using the exponentially modified protein abundance index (emPAI). Finally, this rapid and unbiased PTS protocol was applied to the quantitative analysis of Escherichia coli BW25113 wild-type and relA knock-out (KO) strains.     

Toward the complete membrane proteome: high coverage of integral membrane proteins through transmembrane peptide detection

To attain a comprehensive membrane proteome of two strains of Corynebacterium glutamicum (l-lysine-producing and the characterized model strains), both sample pretreatment and analysis methods were optimized. Isolated bacterial membranes were digested with trypsin/cyanogen bromide or trypsin/chymotrypsin, and a complementary protein set was identified using the multidimensional protein identification technology (MudPIT). Besides a distinct number of cytosolic or membrane-associated proteins, the combined data analysis from both digests yielded 326 integral membrane proteins ( approximately 50% of all predicted) covering membrane proteins both with small and large numbers of transmembrane helices. Also membrane proteins with a high GRAVY score were identified, and basic and acidic membrane proteins were evenly represented. A significant increase in hydrophobic peptides with distinctly higher sequence coverage of transmembrane regions was achieved by trypsin/chymotrypsin digestion in an organic solvent. The percentage of identified membrane proteins increased with protein size, yielding 80% of all membrane proteins above 60 kDa. Most prominently, almost all constituents of the respiratory chain and a high number of ATP-binding cassette transport systems were identified. This newly developed protocol is suitable for the quantitative comparison of membrane proteomes and will be especially useful for applications such as monitoring protein expression under different growth and fermentation conditions in bacteria such as C. glutamicum. Moreover with more than 50% coverage of all predicted membrane proteins (including the non-expressed species) this improved method has the potential for a close-to-complete coverage of membrane proteomes in general.     

Comparison of SDS- and methanol-assisted protein solubilization and digestion methods for Escherichia coli membrane proteome analysis by 2-D LC-MS/MS

Both organic solvent and surfactant have been used for dissolving membrane proteins for shotgun proteomics. In this work, two methods of protein solubilization, namely using 60% methanol or 1% SDS, to dissolve and analyze the inner membrane fraction of an Escherichia coli K12 cell lysate were compared. A total of 358 proteins (1417 unique peptides) from the methanol-solubilized protein mixture and 299 proteins (892 peptides) from the SDS-solubilized sample-were identified by using trypsin digestion and 2-D LC-ESI MS/MS. It was found that the methanol method detected more hydrophobic peptides, resulting in a greater number of proteins identified, than the SDS method. We found that 159 out of 358 proteins (44%) and 120 out of 299 proteins (40%) detected from the methanol- and SDS-solubilized samples, respectively, are integral membrane proteins. Among the 190 integral membrane proteins 70 were identified exclusively in the methanol-solubilized sample, 89 were identified by both methods, and only 31 proteins were exclusively identified by the SDS method. It is shown that the integral membrane proteins reflected the theoretical proteome for number of transmembrane helices, length, functional class, and topology, indicating there was no bias in the proteins identified.     

A combination method of chemical with enzyme reactions for identification of membrane proteins

A simple method for effective analysis of various proteins has been developed, including membrane proteins, with LC-MS/MS, using CNBr and acetic acid cleavage in one reaction for the digestion of both the M/ and /D/ positions within the target proteins. This dual chemical reaction has been compared with traditional CNBr or an acid cleavage method using a rat kidney membrane fraction and it showed an advantage of the dual reaction with respect to a high number of peptides detected and a high protein recovery. Furthermore, when this dual chemical reaction was combined with trypsin digestion, the number of proteins surprisingly increased approximately 3.0 times more than in the cases with the trypsin digestion only. It was also 1.9 times more than in cases dealing with Tube-Gel trypsin digestion, which is one of the most efficient digestion methods. In addition, it was shown that this dual chemical reaction could be applied to an in-gel digestion. Using the combination of the chemical and enzyme reaction, 172 proteins including 95 membrane proteins were identified. This indicated that this method is one of the efficient systems in single MS/MS analysis. In particular, many membrane proteins identified in this study were detected by a new combination, but not by a traditional trypsin digestion method.     

Tube-gel digestion: a novel proteomic approach for high throughput analysis of membrane proteins

This study describes a new protein digestion protocol in which a variety of detergents can be used to solubilize membrane proteins and facilitate trypsin digestion with higher efficiency. In this protocol, proteins are dissolved in solutions containing various detergents and directly incorporated into a polyacrylamide gel matrix without electrophoresis. Detergents are subsequently eliminated from the gel matrix while proteins are still immobilized in the gel matrix. After in-gel digestion of proteins, LC-MS/MS is used to analyze the extracted peptides for protein identification. The uniqueness of the protocol is that it allows usage of a variety of detergents in the starting solution without interfering with LC-MS/MS analysis. We hereby demonstrate that different detergents, including ionic SDS, non-ionic Triton X-100 and n-octyl beta-d-glucopyranoside, and zwitterionic CHAPS, can be used to achieve maximum solubilization of membrane proteins with minimal interference with LC-MS/MS analysis. Enhanced digestions, i.e. improved number and intensity of detected peptides, are also demonstrated for digestion-resistant proteins such as myoglobin, ubiquitin, and bacteriorhodopsin. An additional advantage of the Tube-Gel digestion protocol is that, even without electrophoresis separation, it allows high throughput analysis of complex protein mixtures when coupled with LC-MS/MS. The protocol was used to analyze a complex membrane protein mixture prepared from prostate cancer cells. The protocol involves only a single digestion and 2.5 h of LC-MS/MS analysis and identified 178 membrane proteins. In comparison, the same membrane fraction was resolved by SDS-PAGE, and 20 gel slices were excised and individually digested and analyzed by LC-MS/MS. The more elaborate effort demanded more than 50 h of LC-MS/MS analysis and identified 268 proteins. The new Tube-Gel digestion protocol is an alternative method for high throughput analysis of membrane proteins.     

Comparative study of workflows optimized for in-gel, in-solution, and on-filter proteolysis in the analysis of plasma membrane proteins

Proteomic studies of plasma membrane proteins are challenged by the limited solubility of these proteins and the limited activity of proteolytic enzymes in solubilizing agents such as SDS. In this work, we have evaluated three bottom-up workflows to obtain tryptic peptides from plasma membrane proteins solubilized with 2% SDS. The workflows are in-gel digestion, in-solution digestion, and on-filter digestion. The efficiencies of these strategies, optimized to employ different matrices for trypsin cleavage, were compared using a plasma membrane sample enriched from multiple myeloma cells using a nanoparticle pellicle. On the basis of the number of proteins identified, number of transmembrane proteins identified, hydrophobicity, and spectral count per protein, the workflow that uses in-gel digestion is the most advantageous approach for analysis of plasma membrane proteins.     

Membrane protein identification: N-terminal labeling of nontryptic membrane protein peptides facilitates database searching

Membrane proteins are fairly refractory to digestion especially by trypsin, and less specific proteases, such as elastase and pepsin, are much more effective. However, database searching using nontryptic peptides is much less effective because of the lack of charge localization at the N and C termini and the absence of sequence specificity. We describe a method for N-terminal-specific labeling of peptides from nontryptic digestions of membrane proteins, which facilitates Mascot database searching and can be used for relative quantitation. The conditions for digestion have been optimized to obtain peptides of a suitable length for mass spectrometry (MS) fragmentation. We show the effectiveness of the method using a plasma membrane preparation from a leukemia cell line and demonstrate a large increase in the number of membrane proteins, with small extra-membranar domains being identified in comparison to previous published methods.     

Comparative analysis of OFFGel,strong cation exchange with pH gradient,and RP at high pH for first‐dimensional separation of peptides from a membrane‐enriched protein fraction

The analysis and quantitation of membrane proteins have proved challenging for proteomics. Although several approaches have been introduced to complement gel‐based analysis of intact proteins, the literature is rather limited in comparing major emerging approaches. Peptide fractionation using IEF (OFFGel), strong cation exchange HPLC using a pH gradient (SCX‐pG), and RP HPLC at high pH, have been shown to increase peptide and protein identification over classic MudPIT approaches. This article compares these three approaches for first‐dimensional separation of peptides using a detergent phase (Triton X‐114) enriched membrane fraction from mouse cortical brain tissue. Results indicate that RP at high pH (pH 10) was superior for the identification of more peptides and proteins in comparison to the OFFGel or the SCX‐pG approaches. In addition, gene ontology analysis (GOMiner) revealed that RP at high pH (pH 10) successfully identified an increased number of proteins with “membrane” ontology, further confirming its suitability for membrane protein analysis, in comparison to SCX‐pG and OFFGel techniques.     

Characterization of the rat liver membrane proteome using peptide immobilized pH gradient isoelectric focusing

Membrane proteins are of particular interest in proteomics because of their potential therapeutic utility. Past proteomic approaches used to investigate membrane proteins have only been partially successful at providing a comprehensive analysis due to the inherently hydrophobic nature and low abundance for some of these proteins. Recently, these difficulties have been improved by analyzing membrane protein enriched samples using shotgun proteomics. In addition, the recent application of methanol-assisted trypsin digestion of membrane proteins has been shown to be a method to improve membrane protein identifications. In this study, a comparison of different concentrations of methanol was assessed for assisting membrane protein digestion with trypsin prior to analysis using a gel-based shotgun proteomics approach called peptide immobilized pH gradient isoelectric focusing (IPG-IEF). We demonstrate the use of peptide IEF on pH 3-10 IPG strips as the first dimension of two-dimensional shotgun proteomics for protein identifications from the membrane fraction of rat liver. Tryptic digestion of proteins was carried out in varying concentrations of methanol in 10 mM ammonium bicarbonate: 0% (v/v), 40% (v/v), and 60% (v/v). A total of 800 proteins were identified from 60% (v/v) methanol, which increased the protein identifications by 17% and 14% compared to 0% (v/v) methanol and 40% (v/v) methanol assisted digestion, respectively. In total, 1549 nonredundant proteins were identified from all three concentrations of methanol including 690 (42%) integral membrane proteins of which 626 of these proteins contained at least one transmembrane domain. Peptide IPG-IEF separation of peptides was successful as the peptides were separated into discrete pI regions with high resolution. The results from this study prove utility of 60% (v/v) methanol assisted digestion in conjunction with peptide IPG-IEF as an optimal shotgun proteomics technique for the separation and identification of previously unreported membrane proteins.     

A proteomic approach for investigation of photosynthetic apparatus in plants

The proteome of the photosynthetic apparatus of barley (Hordeum vulgare), obtained by analysis of thylakoids without any previous fractionation, was mapped by native electrophoresis followed by sodium dodecyl sulfate polyacrylamide gel electrophoresis (SDS-PAGE) as the second dimension two-dimensional-blue native (2-D/BN)/SDS-PAGE). This protocol provided an excellent alternative to the 2-D-isoelectric focusing/sodium dodecyl sulfate-polyacrylamide gel electrophoresis for 2-D separation of the most hydrophobic thylakoid proteins. Monocots and dicots showed significant differences in the first dimension while in the second dimension patterns appeared similar. Identification of each spot was performed by internal peptide primary sequence determination using both nano-electrospray ionization tandem mass spectrometry and, to a lesser extent, peptide mass fingerprinting matrix-assisted laser desorption/ionization-time of flight using MALDI-TOF. This is due in particular to the fact that a limited number of peptides was obtained after trypsin digestion of these highly hydrophobic proteins. A larger number of peptides from hydrophilic intermembrane domains of transmembrane proteins were detected. Despite this, about 70% of the expected proteins were identified, including proteins with grand average of hydropathicity scores higher than 0.5. It is therefore reasonable to assert that protein hydrophobicity is not the limiting factor. Small proteins were not well identified with trypsin digestion. Instead some of these could be identified using acid hydrolysis. The method presented here does not require prefractionation of different thylakoid complexes and consequently gives confidence in comparing the proteome of the photosynthetic apparatus before and after treatment. It thus allows us to understand the molecular mechanisms underlying physiological adaptations of higher plants and to perform screening of photosynthetic mutants.     

Identification of membrane proteins from mammalian cell/tissue using methanol-facilitated solubilization and tryptic digestion coupled with 2D-LC-MS/MS

The core prerequisites for an efficient proteome-scale analysis of mammalian membrane proteins are effective isolation, solubilization, digestion and multidimensional liquid chromatography-tandem mass spectrometry (LC-MS/MS). This protocol is for analysis of the mammalian membrane proteome that relies on solubilization and tryptic digestion of membrane proteins in a buffer containing 60% (vol/vol) methanol. Tryptic digestion is followed by strong cation exchange (SCX) chromatography and reversed phase (RP) chromatography coupled online with MS/MS for protein identification. The use of a methanol-based buffer eliminates the need for reagents that interfere with chromatographic resolution and ionization of the peptides (e.g., detergents, chaotropes, inorganic salts). Sample losses are minimized because solubilization and digestion are carried out in a single tube avoiding any sample transfer or buffer exchange between these steps. This protocol is compatible with stable isotope labeling at the protein and peptide level, enabling identification and quantitation of integral membrane proteins. The entire procedure--beginning with isolated membrane fraction and finishing with MS data acquisition--takes 4-5 d.     

多维色谱-串联质谱联用技术分离和鉴定小鼠肝脏质膜蛋白质

采用自动在线纳流多维液相色谱 串联质谱联用的方法分离和鉴定蔗糖密度梯度离心法分离和富集的小鼠肝脏质膜蛋白质 .以强阳离子交换柱为第一相 ,反相柱为第二相 ,在两相之间连接一预柱脱盐和浓缩肽段 .用含去污剂的溶剂提取细胞质膜中的蛋白质 ,获得的质膜蛋白质经酶解和适当的酸化后通过离子交换柱吸附 ,分别用 10个不同浓度的乙酸铵盐溶液进行分段洗脱 .洗脱物经预柱脱盐和浓缩后进入毛细管反相柱进行反相分离 ,分离后的肽段直接进入质谱仪离子源进行一级和二级质谱分析 .质谱仪采得的数据经计算机处理后用Mascot软件进行蛋白质数据库搜寻 ,共鉴定出 12 6种蛋白质 ,其中 4 1种为膜蛋白 ,包括与膜相关的蛋白质和具有多个跨膜区的整合膜蛋白 ,为建立质膜蛋白质组学研究的适宜方法和质膜蛋白质数据库提供了有价值的基础性研究资料 .     

Standardisation of rapid in-gel digestion by mass spectrometry

In-gel digestion has been standardised using a poly(propylene) disposable. We designed a four-step rapid and simple in-gel digestion protocol which is carried out in one self-contained reaction tube avoiding keratin contamination. In order to quantify the efficiency of in-gel digestion, we developed a rapid on-column peptide acetylation protocol. Results show that trypsin in-gel uptake is increased and in-gel digestion is 90% complete within 15 min. We further show that spectrum quality, peptide yield and sequence coverage for mass spectrometric analysis are enhanced. We utilise 2-D PAGE separation of photosystem II from barley to demonstrate that the protocol facilitates identification of highly hydrophobic membrane proteins.     

Proteome profile of human breast cancer tissue generated by LC-ESI-MS/MS combined with sequential protein precipitation and solubilization

Comprehensive proteome profiling of breast cancer tissue samples is challenging, as the tissue samples contain many proteins with varying concentrations and modifications. We report an effective sample preparation strategy combined with liquid chromatography (LC) electrospray ionization (ESI) quadrupole time-of-flight (QTOF) MS/MS for proteome analysis of human breast cancer tissue. The complexity of the breast cancer tissue proteome was reduced by using protein precipitation from a tissue extract, followed by sequential protein solubilization in solvents of different solubilizing strength. The individual fractions of protein mixtures or subproteomes were subjected to trypsin digestion and the resultant peptides were separated by strong cation exchange (SCX) chromatography, followed by reversed-phase capillary LC combined with high resolution and high accuracy ESI-QTOF MS/MS. This approach identified 14407 unique peptides from 3749 different proteins based on peptide matches with scores above the threshold scores at the 95% confidence level in MASCOT database search of the acquired MS/MS spectra. The false positive rate of peptide matches was determined to be 0.95% by using the target-decoy sequence search strategy. On the basis of gene ontology categorization, the identified proteins represented a wide variety of biological functions, cellular processes, and cellular locations.     

Quantitative Assessment of In-solution Digestion Efficiency Identifies Optimal Protocols for Unbiased Protein Analysis

The majority of mass spectrometry-based protein quantification studies uses peptide-centric analytical methods and thus strongly relies on efficient and unbiased protein digestion protocols for sample preparation. We present a novel objective approach to assess protein digestion efficiency using a combination of qualitative and quantitative liquid chromatography-tandem MS methods and statistical data analysis. In contrast to previous studies we employed both standard qualitative as well as data-independent quantitative workflows to systematically assess trypsin digestion efficiency and bias using mitochondrial protein fractions. We evaluated nine trypsin-based digestion protocols, based on standard in-solution or on spin filter-aided digestion, including new optimized protocols. We investigated various reagents for protein solubilization and denaturation (dodecyl sulfate, deoxycholate, urea), several trypsin digestion conditions (buffer, RapiGest, deoxycholate, urea), and two methods for removal of detergents before analysis of peptides (acid precipitation or phase separation with ethyl acetate). Our data-independent quantitative liquid chromatography-tandem MS workflow quantified over 3700 distinct peptides with 96% completeness between all protocols and replicates, with an average 40% protein sequence coverage and an average of 11 peptides identified per protein. Systematic quantitative and statistical analysis of physicochemical parameters demonstrated that deoxycholate-assisted in-solution digestion combined with phase transfer allows for efficient, unbiased generation and recovery of peptides from all protein classes, including membrane proteins. This deoxycholate-assisted protocol was also optimal for spin filter-aided digestions as compared with existing methods.MS-based proteomics is an indispensable technology for the characterization of complex biological systems, including relative or absolute protein expression levels and protein post-translational modifications. The most popular method for analyzing medium to high complexity protein samples in large-scale proteomics relies on protein digestion by using the endoprotease trypsin. Analysis and sequencing of tryptic peptides by liquid chromatography-tandem MS (LC-MS/MS)¹ then enables identification and determination of protein expression levels based on the peptide ion abundance level or the (fragment) ion intensities of identified peptides. This peptide-centric approach thus strongly relies on efficient, unbiased and reproducible protein digestion protocols. Efficiency is required to maximize the number of detectable peptides per protein (coverage) to distinguish unique proteins within protein families with similar sequences and/or sequence variants, and to detect post-translational modifications. Unbiased generation of peptides is required for the resulting data set to most accurately reflect the relative (stoichiometry) and absolute protein abundance in a sample. A particular protocol should be unbiased with respect to abundance, molecular weight, hydrophobicity and protein class. Membrane proteins for example are often suspected to be underrepresented. For MS-based proteomics approaches several critical steps can be distinguished: (a) disruption and solubilization of cells and protein complexes, (b) protein denaturation and enzymatic proteolysis, (c) MS-compatible peptide recovery, which normally entails removal of reagent leftovers and desalting before MS analysis, (d) adequate peptide separation (achieved by liquid chromatography), and (e) MS peptide analysis and sequencing (MS/MS), including the chosen data acquisition strategy.Comparative evaluations of digestion protocols generally consist of qualitative studies using standard tandem mass spectrometry. These approaches may reveal efficiency (i.e. more identifications), but are unable to reveal digestion protocol induced bias with respect to peptide and protein abundance, including membrane proteins. In addition, most data-dependent acquisition workflows are intrinsically biased, which is detrimental for making comparisons. The aim of the present study was to systematically assess efficiency and bias of trypsin-based protocols applying both standard qualitative and label-free quantitative MS approaches.The in-gel digestion protocol for proteomics, established over 15 years ago (1), has been the cornerstone method affording robust protein identifications from many sample types. Although sodium dodecyl sulfate (SDS) interferes with trypsin digestion and hampers LC-MS analysis, this powerful detergent can still be used to achieve complete protein solubilization as gel-separation is an effective way to remove interfering substances. Gel-based approaches are however not optimal for protein samples of increasing complexity and dynamic range (2). Inherent and practical limitations include, for example, concentration-dependent, incomplete peptide recovery and error-prone handling procedures (3–6). This hampers throughput, reproducibility and unbiased protein analysis, which in recent years has prompted a shift toward the application and optimization of in-solution digestion procedures.Previous comparative studies revealed that for in-solution digestions, the acid labile and MS-compatible detergent RapiGest performed most favorably compared with buffer only, urea, other detergents and organic solvents (7–9). Sodium deoxycholate (SDC), naturally found in mammalian bile (10), has emerged as a cheaper MS-compatible detergent for in-solution digestion (11). Unlike other detergents, SDC was found to enhance trypsin activity almost fivefold at a concentration of 1% (12). Like RapiGest, SDC can also be removed by acidification, but potentially without detrimental peptide loss if a phase separation protocol involving organic solvent is applied (12).An alternative strategy is to perform protein digestion on spin filter devices, introduced a few years ago by Manza and co-workers (13), and further developed by Wisniewski et al. (14). This approach allows the use of SDS to first achieve complete protein solubilization followed by removal of the detergent through repeated washes with urea (14). This is an effective way to remove interfering chemicals and small molecules after protein solubilization, and before digestion, without substantial sample loss. Although this protocol is touted to be a highly effective and universal method for any type of sample, digestion is performed using urea or buffer only and has so far not been evaluated in combination with detergents such as SDC.For our comparative study we selected protocols and methods based on spin filter-aided and standard in-solution digestion that were previously reported optimal and we also report novel optimized protocols. We investigated several experimental parameters including reagents for protein solubilization and denaturation (SDS, SDC, urea), spin filter aided removal of SDS before digestion (urea, SDC, buffer), trypsin digestion conditions (buffer, RapiGest, SDC, urea), and methods for removal of detergents before analysis of peptides (acid precipitation or phase separation with ethyl acetate).Mitochondria are organelles carrying out key metabolic processes fundamental for cellular function (15). The mitochondrial proteome is predicted to contain up to a thousand proteins (16) and is very heterogeneous with a wide range of protein pI, molecular weight and hydrophobicity values (17). We selected mitochondrial preparations to serve as model sample of medium complexity, containing a favorable combination of peptide and protein classes, including soluble and insoluble membrane-anchored or integral proteins.Using standard qualitative as well as data-independent quantitative LC-MS/MS workflows we demonstrate that SDC-based protocols combined with phase separation are the most optimal for both in-solution and filter-aided tryptic digestion, yielding the highest efficiency and lowest bias. This workflow enabled quantitative and objective assessment of various protein digestion conditions, identifying optimal protocols for efficient and unbiased protein analysis.     

Tryptic digestion of ubiquitin standards reveals an improved strategy for identifying ubiquitinated proteins by mass spectrometry

Ubiquitination plays an essential role in maintaining cellular homeostasis by regulating a multitude of essential processes. The ability to identify ubiquitinated proteins by MS currently relies on a strategy in which ubiquitinated peptides are identified by a 114.1 Da diglycine (GG) tag on lysine residues, which is derived from the C-terminus of ubiquitin, following trypsin digestion. In the following study, we report a more comprehensive approach for mapping ubiquitination sites by trypsin digestion and MS/MS analysis. We demonstrate that ubiquitination sites can be identified by signature peptides containing a GG-tag (114.1 Da) and an LRGG-tag (383.2 Da) on internal lysine residues as well as a GG-tag found on the C-terminus of ubiquitinated peptides. Application of this MS-based approach enabled the identification of 96 ubiquitination sites from proteins purified from human MCF-7 breast cancer cells, representing a 2.4-fold increase in the number of ubiquitination sites that could be identified over standard methods. Our improved MS-based strategy will aid future studies which aim to identify and/or characterize ubiquitinated proteins in human cells.