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A Novel Chromatographic Method Allows On-line Reanalysis of the Proteome

2008; Elsevier BV; Volume: 7; Issue: 8 Linguagem: Inglês

10.1074/mcp.m800141-mcp200

1535-9484

Leonie F. Waanders, Reinaldo Almeida, S.Lesley Prosser, Juürgen Cox, Daniel Eikel, Mark Allen, Gary A. Schultz, Matthias Mann,

Advanced Proteomics Techniques and Applications

Liquid chromatography combined with electrospray ionization is widely used for direct analysis of polar and labile molecules by LCMS. The on-line coupling in LCMS is a major strength but also causes a principal limitation that each eluting analyte has to be analyzed immediately and is not available for detailed interrogation after the LCMS run. Here we developed a new chromatographic strategy, which removes this limitation. After column separation the flow is split, one portion is analyzed directly, and the other is diverted to a capture capillary. After the direct LCMS run, the flow is switched, and the portion stored in the capillary is analyzed (“replay run”). We describe a setup consisting of an analytical column, a splitting valve, and a focusing column, which performs at full sensitivity and undiminished chromatographic resolution. We demonstrate three principal advantages of this system: nearly continuous MS utilization, duplicate analysis without requirement for additional sample, and targeting of important but undersampled features in the replay run. Liquid chromatography combined with electrospray ionization is widely used for direct analysis of polar and labile molecules by LCMS. The on-line coupling in LCMS is a major strength but also causes a principal limitation that each eluting analyte has to be analyzed immediately and is not available for detailed interrogation after the LCMS run. Here we developed a new chromatographic strategy, which removes this limitation. After column separation the flow is split, one portion is analyzed directly, and the other is diverted to a capture capillary. After the direct LCMS run, the flow is switched, and the portion stored in the capillary is analyzed (“replay run”). We describe a setup consisting of an analytical column, a splitting valve, and a focusing column, which performs at full sensitivity and undiminished chromatographic resolution. We demonstrate three principal advantages of this system: nearly continuous MS utilization, duplicate analysis without requirement for additional sample, and targeting of important but undersampled features in the replay run. The development of electrospray mass spectrometry has allowed analysis directly from the liquid phase (1Fenn J.B. Mann M. Meng C.K. Wong S.F. Whitehouse C.M. Electrospray ionization for mass spectrometry of large biomolecules.Science. 1989; 246: 64-71Crossref PubMed Scopus (6380) Google Scholar). This feature of electrospray makes it eminently suitable for the on-line coupling of separation and ionization before MS analysis. In nanoscale LCMS analyte species are concentrated into very small volumes, increasing sensitivity. Furthermore the excellent separation capacity of high performance chromatographic systems is multiplied with the high resolution of modern mass spectrometers, resulting in exceptional combined separation power (2Hernandez-Borges J. Aturki Z. Rocco A. Fanali S. Recent applications in nanoliquid chromatography.J. Sep. Sci. 2007; 30: 1589-1610Crossref PubMed Scopus (121) Google Scholar). Small molecules, peptides, and proteins are routinely analyzed by this powerful technology. However, compared with off-line methods such as nanoelectrospray (3Wilm M. Mann M. Analytical properties of the nanoelectrospray ion source.Anal. Chem. 1996; 68: 1-8Crossref PubMed Scopus (1719) Google Scholar) or MALDI (4Karas M. Hillenkamp F. Laser desorption ionization of proteins with molecular masses exceeding 10,000 daltons.Anal. Chem. 1988; 60: 2299-2301Crossref PubMed Scopus (4850) Google Scholar), on-line coupling also has some inherent drawbacks. The short time during elution of a peak requires a fast and automatic decision on which peak to sequence. In complex mixtures, many peptides co-elute, and some may not be sequenced at all (5Kuster B. Schirle M. Mallick P. Aebersold R. Scoring proteomes with proteotypic peptide probes.Nat. Rev. Mol. Cell Biol. 2005; 6: 577-583Crossref PubMed Scopus (306) Google Scholar). Peptides of special interest, for example, those with regulatory post-translational modifications, should be characterized in depth, but the fact that they are important may only become evident after the analysis. Some of these drawbacks can in principle be addressed by slowing down the flow (“peak parking” (6Davis M.T. Stahl D.C. Hefta S.A. Lee T.D. A microscale electrospray interface for on-line, capillary liquid chromatography/tandem mass spectrometry of complex peptide mixtures.Anal. Chem. 1995; 67: 4549-4556Crossref PubMed Scopus (200) Google Scholar)), fraction collection, or repeat injection. However, none of these methods is ideal from an analytical standpoint. Peak parking is of limited utility for complex mixtures because the flow may have to be stopped every few seconds, and the run would be extended to impractical lengths. Fraction collection is useful in many instances, but at very low flow rates it is less practical because of the low volume of fractions. In nanoflow LC peptides typically elute in about 50 nl (based on an elution time of 15 s using a 200 nl/min flow rate). To handle these fractions one would need ∼1 μl of sample, but adding buffer reduces the concentration 20-fold causing a dramatic loss of signal intensity. Repeat injections multiply total required analysis time and may not be optimal if sample is limited because reinjection consumes twice as much sample. We wished to develop a novel concept in LCMS that would allow targeted measurement of analyte mixtures without compromising sensitivity or chromatographic performance while requiring little or no additional time. Because electrospray is a concentration-dependent process and therefore maintains full signal at decreased flow rates, we and others previously developed splitting systems in which the column effluent was directed to MS analysis as well as to a fraction collector to enable the reanalysis of chromatographic fractions (7Staack R.F. Varesio E. Hopfgartner G. The combination of liquid chromatography/tandem mass spectrometry and chip-based infusion for improved screening and characterization of drug metabolites.Rapid Commun. Mass Spectrom. 2005; 19: 618-626Crossref PubMed Scopus (43) Google Scholar, 8Corso T.N. Van Pelt C.K. Li J. Ptak C. Huang X. Ultralow-volume fraction collection from NanoLC columns for mass spectrometric analysis of protein phosphorylation and glycosylation.Anal. Chem. 2006; 78: 2209-2219Crossref PubMed Scopus (14) Google Scholar). However, at very low flow rates, fraction collection became increasingly difficult, prompting us to explore alternative ways of storing the chromatographically separated sample. Here we describe a novel setup in which we collect part of a column effluent in a long capture capillary that we reanalyze after the direct run. In this study we describe the new concept and evaluate the system in terms of chromatographic and mass spectrometric performance. Furthermore we show the applicability to a complex proteomics sample and demonstrate a useful application: targeting important peptides that were not characterized in sufficient detail in the direct run. A “head to head” and exhaustive comparison with other possible LCMS setups or MALDI methods is not the subject of this study. We constructed the “RePlay system” consisting of a six-port splitting valve, a flow sensor, a long capillary serving as a capture capillary, and short capillaries to adjust the split ratio (see Fig. 1). The splitting valve was specially constructed for accurate flow ratios and extremely low dead volumes at nl/min flow rates (Advion BioSystems, Ithaca, NY). LC was performed on a Nano-HPLC 1200 system (Agilent, Waldbronn, Germany) with a 10-cm-long 75-μm-inner diameter IntegraFrit™ ProteoPepII analytical column (5-μm RP-C18 resin, New Objective, Woburn, MA) coupled to the RePlay valve in which the flow was split. The gradients were essentially as described previously (12Olsen J.V. Ong S.E. Mann M. Trypsin cleaves exclusively C-terminal to arginine and lysine residues.Mol. Cell. Proteomics. 2004; 3: 608-614Abstract Full Text Full Text PDF PubMed Scopus (881) Google Scholar) with peptides eluting from 13 to 60% solvent B (0.5% acetic acid in 80% acetonitrile). One part of the effluent was directed to a 7-cm in-house pulled 75-μm-inner diameter fused silica emitter packed with ReproSil-Pur C18-AQ 3-μm resin (Dr. Maisch GmbH, Ammerbuch-Entringen, Germany), termed the “focusing column” for direct on-line LCMS analysis on an LTQ-Orbitrap mass spectrometer (Thermo Fisher Scientific, Bremen, Germany). Meanwhile the second part of the effluent was collected in the fused silica capture capillary of typically 13-m length and 30-μm inner diameter. The capture line (Composite Metal Services Ltd., Shipley, UK) was capable of storing around 10 μl, appropriate for a 100-min gradient at an effective flow rate of 100 nl/min. For the 30-min gradient a 3-m capillary was used. This stored gradient was then directed to the same 7-cm pulled column by valve switching triggered from the MS acquisition software. Split adjusters, 10-μm-inner diameter capillaries (Composite Metal Services Ltd.), were cut to the length resulting in the desired split ratio. These split adjusters needed to be fine tuned whenever the focusing column was replaced. We recommend to carefully tighten, not to overtighten, these capillaries because we found that small glass particles easily clog the capillaries with a small inner diameter (used as split adjusters). For calculation of the theoretical peak broadening we used the “capillary flow calculator” option of the “Molecular Weight Calculator” freely available as open source software (alchemistmatt). This program calculates the width of the peak as a consequence of diffusion when inserting the initial peak width, the length and inner diameter of the capillary, and the flow rate. Frozen mouse liver tissue was homogenized and in-solution digested by trypsin as described previously (9Shi R. Kumar C. Zougman A. Zhang Y. Podtelejnikov A. Cox J. Wisniewski J.R. Mann M. Analysis of the mouse liver proteome using advanced mass spectrometry.J. Proteome Res. 2007; 6: 2963-2972Crossref PubMed Scopus (79) Google Scholar), desalted and concentrated on in-house prepared StageTips (10Rappsilber J. Ishihama Y. Mann M. Stop and go extraction tips for matrix-assisted laser desorption/ionization, nanoelectrospray, and LC/MS sample pretreatment in proteomics.Anal. Chem. 2003; 75: 663-670Crossref PubMed Scopus (1833) Google Scholar), and eluted for LCMS analysis. With a split ratio of 1:1, we ran a 100-min gradient (100 nl/min to MS) and reanalyzed the sample in another 100 min (100 nl/min). We also split 3:1 (direct:replay), used a 100-min direct gradient (200 nl/min to MS), and reanalyzed the sample in 35 min (200 nl/min). During the replay run the LC system loaded the next sample on the analytical column. The run was analyzed by in-house developed MaxQuant software (version 1.07.5) essentially as described previously (11Graumann J. Hubner N.C. Kim J.B. Ko K. Moser M. Kumar C. Cox J. Schoeler H. Mann M. Stable isotope labeling by amino acids in cell culture (SILAC) and proteome quantitation of mouse embryonic stem cells to a depth of 5,111 proteins.Mol. Cell. Proteomics. 2007; 7: 672-683Abstract Full Text Full Text PDF PubMed Scopus (243) Google Scholar). The data were searched using Mascot (version 2.1.04, Matrix Science Ltd., London, UK) against the mouse International Protein Index database (version 3.37) supplemented with frequently observed contaminants and concatenated with reversed copies of all sequences (2 × 51,467 entries). Enzyme specificity was set to trypsin, allowing for cleavage N-terminal to proline and between aspartic acid and proline (12Olsen J.V. Ong S.E. Mann M. Trypsin cleaves exclusively C-terminal to arginine and lysine residues.Mol. Cell. Proteomics. 2004; 3: 608-614Abstract Full Text Full Text PDF PubMed Scopus (881) Google Scholar). Carbamidomethylcysteine was set as a fixed modification, and N-acetylation and methionine oxidation were set as variable modifications. The initial maximum allowed mass deviation (13Zubarev R. Mann M. On the proper use of mass accuracy in proteomics.Mol. Cell. Proteomics. 2007; 6: 377-381Abstract Full Text Full Text PDF PubMed Scopus (145) Google Scholar) was set to 5 ppm for monoisotopic precursor ions and 0.5 Da for MS/MS peaks. Maximally three missed cleavages were allowed. The false positive rate at the peptide level and false discovery rate at the protein level were set to 1%, and the required minimum peptide length was 6 amino acids. If the identified peptide sequence set of one protein was equal to or contained the peptide set of another protein, these two proteins were grouped together by MaxQuant, and they were not counted as independent protein hits. Proteins were considered identified when at least two peptides were identified (of which one was uniquely assignable to the respective sequence). His6-SUMO-2 1The abbreviations used are: SUMO, small ubiquitin-like modifier; HCD, higher energy collision dissociation. conjugates were purified as described previously (14Matic I. van Hagen M. Schimmel J. Macek B. Ogg S.C. Tatham M.H. Hay R.T. Lamond A.I. Mann M. Vertegaal A.C. In vivo identification of human small ubiquitin-like modifier polymerization sites by high accuracy mass spectrometry and an in vitro to in vivo strategy.Mol. Cell. Proteomics. 2008; 7: 132-144Abstract Full Text Full Text PDF PubMed Scopus (226) Google Scholar). The samples were subsequently digested by trypsin and concentrated on in-house made StageTips (10Rappsilber J. Ishihama Y. Mann M. Stop and go extraction tips for matrix-assisted laser desorption/ionization, nanoelectrospray, and LC/MS sample pretreatment in proteomics.Anal. Chem. 2003; 75: 663-670Crossref PubMed Scopus (1833) Google Scholar). After measuring the direct run with a “top 10” method using fragmentation of the 10 most abundant ions in the ion trap, a peak list was created with MaxQuant software (version 1.07.5) using default parameters. This list was screened for precursors that when fragmented showed ions with m/z corresponding to SUMO-2 b-ions in the range of b5–b18. Of the precursors that had more than three fragment matches and a total mass larger than a free SUMO-2 peptide, the highest expected isotope peak was added to an inclusion list. In the replay run only these ions were sequenced by use of higher collision dissociation (HCD) fragmentation (15Olsen J.V. Macek B. Lange O. Makarov A. Horning S. Mann M. Higher-energy C-trap dissociation for peptide modification analysis.Nat. Methods. 2007; 4: 709-712Crossref PubMed Scopus (730) Google Scholar). We deselected charge state, precursor mass screening, and dynamic exclusion and fragmented all ions matching an inclusion list item with a 30-ppm tolerance and with a minimum intensity of 30,000. These high resolution fragmentation spectra were validated manually. In a first iteration of our systems we used a storage capillary instead of the fraction collector, and we reversed the flow for reanalysis of the stored gradient. This arrangement inverted the order of the elution and resulted in good resolution of late eluting peaks (those stored in the capillary for a short time) but not of early eluting peaks (supplemental Fig. 1). To enable first in first out analysis, we combined the functions of flow splitting and redirection of the flow into a single device, a low flow, low dead volume splitting valve (Fig. 1). Finally to prevent possible deterioration of chromatographic performance in the second run due to diffusion in the capture capillary, we introduced a second “focusing” column prior to the electrospray emitter. We termed this system “RePlay.” The effluent from the analytical column was split in the appropriate, fixed ratio for direct analysis in the mass spectrometer and for storage in a capture capillary (Fig. 1A). At the end of the gradient, the valve was switched, and the stored gradient separation was eluted through the same focusing column as in the direct mode (Fig. 1B). We tested the performance of the RePlay system (Advion BioSystems, Ithaca, NY) with a BSA standard (Sigma-Aldrich). As shown in Fig. 2, peak intensity and chromatographic resolution were very similar between direct and RePlay analysis with no deterioration over the gradient (Fig. 2C). The fact that the signal in electrospray is concentration-dependent rather than dependent on total analyte amount readily explains this feature of the RePlay setup. We tested different split ratios of the total flow (typically 200 nl/min) between the direct and replay runs from 1:4 to 3:1 and found that the chromatographic performance was excellent with splits in this range. For the experiments reported in this study, we chose a split ratio of 1:1 or 3:1 to keep the volume of the capture capillary small and RePlay analysis time short. To test for potential detrimental effects of diffusion, we varied the inner diameter of the capillary between 20 and 40 μm and stored the gradient in the capture capillary for up to 30 min. Theoretically using a flow rate of 100 nl/min, a peak of 20 s measured at the base would diffuse into 33 s in a 20-μm-inner diameter capillary, whereas the same peak would broaden to 45 s in a 30-μm-inner diameter tubing and to 57 s in a capillary of 40-μm inner diameter. All data presented in this study were acquired using a 30-μm inner diameter capture capillary, and for this capillary no significant influence on chromatographic performance was observed. This indicates that the diffusion can still be reversed by the focusing column under these conditions. However, when we did not use the focusing column we indeed observed appreciable peak broadening. Figs. 2, A and B, and 4A illustrate one of the advantages of the RePlay system compared with the routine work flow in our laboratory. During the replay run, the analytical column is re-equilibrated and loaded with a new sample. Thus, the mass spectrometer is continuously sequencing peptides, and the loading and washing steps do not subtract from the duty cycle of MS utilization. As shown in Fig. 2C, four runs were analyzed in 8 × 30 min with essentially 100% duty cycle, whereas without RePlay, the duty cycle is about 50%. For 100-min gradients we accomplished a duty cycle of 90% by directing one-quarter of the flow to the capture capillary and pushing the gradient out 3 times faster (see Fig. 4). However, to ensure continued high chromatographic resolution we found it advantageous to include a wash and equilibration of the focusing column for a few minutes in all protocols. Next we characterized the performance of the RePlay system for complex peptide mixtures typical of proteomics experiments. We loaded slightly less than 1 μg of mouse liver tryptic digest, corresponding to less than 20,000 hepatocyte cells, onto the RePlay system. Analysis was performed with a 100-min gradient by a standard “top 5” method on the LTQ-Orbitrap as routinely used in our laboratory (16Olsen J.V. de Godoy L.M. Li G. Macek B. Mortensen P. Pesch R. Makarov A. Lange O. Horning S. Mann M. Parts per million mass accuracy on an Orbitrap mass spectrometer via lock mass injection into a C-trap.Mol. Cell. Proteomics. 2005; 4: 2010-2021Abstract Full Text Full Text PDF PubMed Scopus (1246) Google Scholar). The base peak chromatogram in Fig. 3 shows that the peptide pattern is largely indistinguishable between the direct and replay runs. Peaks eluted on average within 15 s in the direct run and 16 s in the replay run (with standard deviations of 5 and 7 s, respectively; see Fig. 3B). This is as good or better a performance than our standard one-column setup for proteomics experiments. At a false discovery rate of 1%, 6,535 fully tryptic peptides were identified in the direct run, and 5,936 were identified in the replay run, documenting the high reproducibility between the runs. A total of 8,383 unique peptides were identified in the combined analysis. Although this experiment was meant to investigate reproducibility, the replay run nevertheless added 1,848 peptides (28%) not identified in the direct run. On the protein level, the RePlay system identified 1,093 proteins with two unique peptides and at a false discovery rate of 1%, demonstrating that it is well suited to complex proteomics samples. This performance will likely further improve if the mass spectrometer is programmed to sequence only peptides in the replay run that have not been sequenced in the direct run. To demonstrate the ability of reanalyzing a complex mixture without adding to total analysis time, we split one-quarter of the flow into the capture capillary (Fig. 4). The total flow was 270 nl/min during direct analysis (200 nl/min to the focusing column) that lasted for 100 min. During the replay run the flow to the focusing column was also 200 nl/min, “squeezing” the reanalysis into 35 min. Fig. 4, B and C, show that this regime preserved peak intensities and slightly sharpened chromatographic peaks. Note that total analysis time was 150 min, very close to the 140-min standard cycle used in our laboratory in which peptides elute for about 100 min. On-line reanalysis also allows targeting important peptides that were missed or unidentified in the direct analysis. We demonstrate this principle by targeted reanalysis of peptides that are extremely difficult to identify by tandem mass spectrometry. In our work investigating the conjugation of substrates with ubiquitin family proteins, we looked for specific proteins that are in vivo sumoylated by SUMO-2 (14Matic I. van Hagen M. Schimmel J. Macek B. Ogg S.C. Tatham M.H. Hay R.T. Lamond A.I. Mann M. Vertegaal A.C. In vivo identification of human small ubiquitin-like modifier polymerization sites by high accuracy mass spectrometry and an in vitro to in vivo strategy.Mol. Cell. Proteomics. 2008; 7: 132-144Abstract Full Text Full Text PDF PubMed Scopus (226) Google Scholar). Unlike ubiquitin, SUMO-2 leaves a large 32- or 34-amino acid peptide on the substrate peptide after tryptic digest, making it highly charged. The complex fragmentation spectra of the cross-linked peptides are notoriously difficult to identify with low resolution data (17Pedrioli P.G. Raught B. Zhang X.D. Rogers R. Aitchison J. Matunis M. Aebersold R. Automated identification of SUMOylation sites using mass spectrometry and SUMmOn pattern recognition software.Nat. Methods. 2006; 3: 533-539Crossref PubMed Scopus (102) Google Scholar). For confident identification of the sumoylated peptide sequence, confirmation of high resolution and high accuracy data is required. To identify these conjugated SUMO-2 peptides in a streamlined fashion we purified His6-SUMO-2 conjugates from HeLa lysate and measured them in the standard way in the direct run. Low resolution fragmentation spectra from the linear ion trap that indicated possible SUMO-2-conjugated peptides were then targeted in the replay run. In this run we only targeted these potential substrate peptides, fragmented them by HCD (15Olsen J.V. Macek B. Lange O. Makarov A. Horning S. Mann M. Higher-energy C-trap dissociation for peptide modification analysis.Nat. Methods. 2007; 4: 709-712Crossref PubMed Scopus (730) Google Scholar), and analyzed them with high resolution and mass accuracy in the orbitrap instead of in the ion trap. Note that this analysis is slower and less sensitive and therefore could not have been performed efficiently in the direct run. Fig. 5 shows the setup of the experiment as well as results for a SUMO-2-conjugated peptide. In the replay run, but not in the direct run, charge states and fragment masses are determined with very high accuracy (Fig. 5D, inset). Interestingly the ion trap CID did not fragment the crucial substrate part of the cross-linked peptide (Fig. 5B); therefore reanalysis with a different fragmentation method (HCD) was especially beneficial in this case (Fig. 5D). The RePlay analysis produced an essentially complete run of y-ions of the substrate peptide. This experiment was performed with a 3:1 split ratio where the RePlay analysis was kept entirely within the time usually needed for washing and loading but that would suffice for characterizing a handful of interesting peptides. In this way, the mass spectrometer could, instead of standing idle, acquire targeted and very high quality data “for free.” In summary, we have demonstrated that the RePlay system enables very efficient use of the mass spectrometer, which is an important advantage given the high demand on sequencing time in large scale proteomics laboratories and the costs of high resolution mass spectrometers. We also demonstrated a “targeted analysis” in which the replay run enabled the collection of crucial, complementary data, thereby dramatically enhancing the information obtained in the direct run.