A Collision-Induced Dissociation Cleavable Isobaric Tag for Peptide Fragment Ion-Based Quantification in Proteomics

Quantifying peptides based on unique peptide fragment ions avoids the issue of ratio distortion that is commonly observed for reporter ion-based quantification approaches. Herein, we present a collision-induced dissociation-cleavable, isobaric acetyl-isoleucine-proline-glycine (Ac-IPG) tag, which conserves the merits of quantifying peptides based on unique fragments while reducing the complexity of the b-ion series compared to conventional fragment ion-based quantification methods thus facilitating data processing. Multiplex labeling is based on selective N-terminal dimethylation followed by derivatization of the ε-amino group of the C-terminal Lys residue of LysC peptides with isobaric Ac-IPG tags having complementary isotope distributions on Pro-Gly and Ac-Ile. Upon fragmentation between Ile and Pro, the resulting y ions, with the neutral loss of Ac-Ile, can be distinguished between the different labeling channels based on different numbers of isotope labels on the Pro-Gly part and thus contain the information for relative quantification, while b ions of different labeling channels have the same m/z values. The proteome quantification capability of this method was demonstrated by triplex labeling of a yeast proteome spiked with bovine serum albumin (BSA) over a 10-fold dynamic range. With the yeast proteins as the background, BSA was detected at ratios of 1.14:5.06:9.78 when spiked at 1:5:10 ratios. The raw mass data is available on the ProteomeXchange with the identifier PXD 018790

Enhanced Sample Multiplexing of Tissues Using Combined Precursor Isotopic Labeling and Isobaric Tagging (cPILOT)

There is an increasing demand to analyze many biological samples for disease understanding and biomarker discovery. Quantitative proteomics strategies that allow simultaneous measurement of multiple samples have become widespread and greatly reduce experimental costs and times. Our laboratory developed a technique called combined precursor isotopic labeling and isobaric tagging (cPILOT), which enhances sample multiplexing of traditional isotopic labeling or isobaric tagging approaches. Global cPILOT can be applied to samples originating from cells, tissues, bodily fluids, or whole organisms and gives information on relative protein abundances across different sample conditions. cPILOT works by 1) using low pH buffer conditions to selectively dimethylate peptide N-termini and 2) using high pH buffer conditions to label primary amines of lysine residues with commercially-available isobaric reagents (see Table of Materials/Reagents). The degree of sample multiplexing available is dependent on the number of precursor labels used and the isobaric tagging reagent. Here, we present a 12-plex analysis using light and heavy dimethylation combined with six-plex isobaric reagents to analyze 12 samples from mouse tissues in a single analysis. Enhanced multiplexing is helpful for reducing experimental time and cost and more importantly, allowing comparison across many sample conditions (biological replicates, disease stage, drug treatments, genotypes, or longitudinal time-points) with less experimental bias and error. In this work, the global cPILOT approach is used to analyze brain, heart, and liver tissues across biological replicates from an Alzheimer's disease mouse model and wild-type controls. Global cPILOT can be applied to study other biological processes and adapted to increase sample multiplexing to greater than 20 samples

Stable isotopic labeling in proteomics

Labeling of proteins and peptides with stable heavy isotopes (deuterium, carbon-13, nitrogen-15, and oxygen-18) is widely used in quantitative proteomics. These are either incorporated metabolically in cells and small organisms, or postmetabolically in proteins and peptides by chemical or enzymatic reactions. Only upon measurement with mass spectrometers holding sufficient resolution, light, and heavy labeled peptide ions or reporter peptide fragment ions segregate and their intensity values are subsequently used for quantification. Targeted use of these labels or mass tags further leads to specific monitoring of diverse aspects of dynamic proteomes. In this review article, commonly used isotope labeling strategies are described, both for quantitative differential protein profiling and for targeted analysis of protein modifications

Selective Maleylation-Directed Isobaric Peptide Termini Labeling for Accurate Proteome Quantification

Isobaric peptide termini labeling (IPTL) is an attractive protein quantification method because it provides more accurate and reliable quantification information than traditional isobaric labeling methods (e.g., TMT and iTRAQ) by making use of the entire fragment-ion series instead of only a single reporter ion. The multiplexing capacity of published IPTL implementations is, however, limited to three. Here, we present a selective maleylation-directed isobaric peptide termini labeling (SMD-IPTL) approach for quantitative proteomics of LysC protein digestion. SMD-IPTL extends the multiplexing capacity to 4-plex with the potential for higher levels of multiplexing using commercially available 13C/15N labeled amino acids. SMD-IPTL is achieved in a one-pot reaction in three consecutive steps: (1) selective maleylation at the N-terminus; (2) labeling at the ϵ-NH2 group of the C-terminal Lys with isotopically labeled acetyl-alanine; (3) thiol Michael addition of an isotopically labeled acetyl-cysteine at the maleylated N-terminus. The isobarically labeled peptides are fragmented into sets of b- and y-ion clusters upon LC-MS/MS, which convey not only sequence information but also quantitative information for every labeling channel and avoid the issue of ratio distortion observed with reporter-ion-based approaches. We demonstrate the SMD-IPTL approach with a 4-plex labeled sample of bovine serum albumin (BSA) and yeast lysates mixed at different ratios. With the use of SMD-IPTL for labeling and a narrow precursor isolation window of 0.8 Th with an offset of -0.2 Th, accurate ratios were measured across a 10-fold mixing range of BSA in a background of yeast proteome. With the yeast proteins mixed at ratios of 1:5:1:5, BSA was detected at ratios of 0.94:2.46:4.70:9.92 when spiked at 1:2:5:10 ratios with an average standard deviation of peptide ratios of 0.34

Quantitative mass spectrometry-based proteomics: An overview

In recent decades, mass spectrometry has moved more than ever before into the front line of protein-centered research. After being established at the qualitative level, the more challenging question of quantification of proteins and peptides using mass spectrometry has become a focus for further development. In this chapter, we discuss and review actual strategies and problems of the methods for the quantitative analysis of peptides, proteins, and finally proteomes by mass spectrometry. The common themes, the differences, and the potential pitfalls of the main approaches are presented in order to provide a survey of the emerging field of quantitative, mass spectrometry-based proteomics

Approaches for Improved Positional Proteomics

Positional proteomics is emerging as an attractive technique to characterize protein termini, which play important biological roles in cells. Even with the advances in past decades, there still are areas for improvement. This thesis focuses on improving data quality and assignment confidence in positional proteomics. A novel workflow was designed for the large-scale identification of protein N-terminal sequences. 4-sulfophenyl isothiocyanate (SPITC) is used for N-termini sulfonation; Upon higher energy collisional dissociation (HCD), SPITC peptides in electrospray ionization ESI generate predominately y-type ion series; such simplification of spectra enables the identification of N-termini with high fidelity. The presence of b1 + SPITC product ions upon HCD furthers the confidence for N-terminal identifications. Secondly, sulfonated N-terminal peptides possess one negative charge site at low pH, which was exploited to enrich the SPITC modified N-terminal peptides by electrostatic repulsion hydrophilic interaction (ERLIC) chromatography. Such enrichment process allows both N-termini enriched and N-termini deficient fractions to be collected and analyzed by LC-MS/MS. This method was applied to an E. coli cell lysate, identifying approximately 350 N-terminal peptides (85% represented neo-N-termini from protein degradation and 15% from leading methionine excision). These N-terminal peptides represented 274 distinct E.coli proteins, 224 of which were also identified in the analysis of flow-through fractions from internal peptides. Another approach we took to boost the identification confidence is by exploiting iTRAQ (isobaric tag for relative and absolute quantitation) in the positional proteomics workflow. This approach allows for multiplexed comparison between different samples, and thus is well-suited for degradadomics analyses where degraded samples are compared to control samples. Both control and protease treated sample are labeled by different tags which allows direct comparison of protein N-termini with neo-N-termini. In addition, samples are analyzed duplicate by labeling with two tags, aiming for quick validation of peptides by internal replicates. In this study, Asp-N digested E.coli cell lysate is taken as a model system. A total of 500 N-terminal peptides, corresponding to 370 proteins, were identified with high confidence in one experiment, with 87% of those proteolytic products matching the expected protease digestion specificity, validating the assignment accuracy of this approach

Approaches for Improved Positional Proteomics

Positional proteomics is emerging as an attractive technique to characterize protein termini, which play important biological roles in cells. Even with the advances in past decades, there still are areas for improvement. This thesis focuses on improving data quality and assignment confidence in positional proteomics. A novel workflow was designed for the large-scale identification of protein N-terminal sequences. 4-sulfophenyl isothiocyanate (SPITC) is used for N-termini sulfonation; Upon higher energy collisional dissociation (HCD), SPITC peptides in electrospray ionization ESI generate predominately y-type ion series; such simplification of spectra enables the identification of N-termini with high fidelity. The presence of b1 + SPITC product ions upon HCD furthers the confidence for N-terminal identifications. Secondly, sulfonated N-terminal peptides possess one negative charge site at low pH, which was exploited to enrich the SPITC modified N-terminal peptides by electrostatic repulsion hydrophilic interaction (ERLIC) chromatography. Such enrichment process allows both N-termini enriched and N-termini deficient fractions to be collected and analyzed by LC-MS/MS. This method was applied to an E. coli cell lysate, identifying approximately 350 N-terminal peptides (85% represented neo-N-termini from protein degradation and 15% from leading methionine excision). These N-terminal peptides represented 274 distinct E.coli proteins, 224 of which were also identified in the analysis of flow-through fractions from internal peptides. Another approach we took to boost the identification confidence is by exploiting iTRAQ (isobaric tag for relative and absolute quantitation) in the positional proteomics workflow. This approach allows for multiplexed comparison between different samples, and thus is well-suited for degradadomics analyses where degraded samples are compared to control samples. Both control and protease treated sample are labeled by different tags which allows direct comparison of protein N-termini with neo-N-termini. In addition, samples are analyzed duplicate by labeling with two tags, aiming for quick validation of peptides by internal replicates. In this study, Asp-N digested E.coli cell lysate is taken as a model system. A total of 500 N-terminal peptides, corresponding to 370 proteins, were identified with high confidence in one experiment, with 87% of those proteolytic products matching the expected protease digestion specificity, validating the assignment accuracy of this approach

Strategies for Proteome-Wide Quantification of Glycosylation Macro- and Micro-Heterogeneity

Protein glycosylation governs key physiological and pathological processes in human cells. Aberrant glycosylation is thus closely associated with disease progression. Mass spectrometry (MS)-based glycoproteomics has emerged as an indispensable tool for investigating glycosylation changes in biological samples with high sensitivity. Following rapid improvements in methodologies for reliable intact glycopeptide identification, site-specific quantification of glycopeptide macro- and micro-heterogeneity at the proteome scale has become an urgent need for exploring glycosylation regulations. Here, we summarize recent advances in N- and O-linked glycoproteomic quantification strategies and discuss their limitations. We further describe a strategy to propagate MS data for multilayered glycopeptide quantification, enabling a more comprehensive examination of global and site-specific glycosylation changes. Altogether, we show how quantitative glycoproteomics methods explore glycosylation regulation in human diseases and promote the discovery of biomarkers and therapeutic targets