Quantify Protein Phosphorylation Research Articles

Fast and deep phosphoproteome analysis with the Orbitrap Astral mass spectrometer

Owing to its roles in cellular signal transduction, protein phosphorylation plays critical roles in myriad cell processes. That said, detecting and quantifying protein phosphorylation has remained a challenge. We describe the use of a novel mass spectrometer (Orbitrap Astral) coupled with data-independent acquisition (DIA) to achieve rapid and deep analysis of human and mouse phosphoproteomes. With this method, we map approximately 30,000 unique human phosphorylation sites within a half-hour of data collection. The technology is benchmarked to other state-of-the-art MS platforms using both synthetic peptide standards and with EGF-stimulated HeLa cells. We apply this approach to generate a phosphoproteome multi-tissue atlas of the mouse. Altogether, we detect 81,120 unique phosphorylation sites within 12 hours of measurement. With this unique dataset, we examine the sequence, structural, and kinase specificity context of protein phosphorylation. Finally, we highlight the discovery potential of this resource with multiple examples of phosphorylation events relevant to mitochondrial and brain biology.

An Optimized Single-Molecule Pull-Down Assay for Quantification of Protein Phosphorylation.

Phosphorylation is a necessary posttranslational modification that regulates protein function and directs cell signaling outcomes. Current methods to measure protein phosphorylation cannot preserve the heterogeneity in phosphorylation across individual proteins. The single-molecule pull-down (SiMPull) assay was developed to investigate the composition of macromolecular complexes via immunoprecipitation of proteins on a glass coverslip followed by single-molecule imaging. The current technique is an adaptation of SiMPull that provides robust quantification of the phosphorylation state of full-length membrane receptors at the single-molecule level. Imaging thousands of individual receptors in this way allows for quantifying protein phosphorylation patterns. The present protocol details the optimized SiMPull procedure, from sample preparation to imaging. Optimization of glass preparation and antibody fixation protocols further enhances data quality. The current protocol provides code for the single-molecule data analysis that calculates the fraction of receptors phosphorylated within a sample. While this work focuses on phosphorylation of the epidermal growth factor receptor (EGFR), the protocol can be generalized to other membrane receptors and cytosolic signaling molecules.

Global Phosphoproteome Analysis Using High-Field Asymmetric Waveform Ion Mobility Spectrometry on a Hybrid Orbitrap Mass Spectrometer.

Mass spectrometry is the premier tool for identifying and quantifying protein phosphorylation on a global scale. Analysis of phosphopeptides requires enrichment, and even after the samples remain highly complex and exhibit broad dynamic range of abundance. Achieving maximal depth of coverage for phosphoproteomics therefore typically necessitates offline liquid chromatography prefractionation, a time-consuming and laborious approach. Here, we incorporate a recently commercialized aerodynamic high-field asymmetric waveform ion mobility spectrometry (FAIMS) device into the phosphoproteomic workflow. We characterize the effects of phosphorylation on the FAIMS separation, describe optimized compensation voltage settings for unlabeled phosphopeptides, and demonstrate the advantages of FAIMS-enabled gas-phase fractionation. Standard FAIMS single-shot analyses identified around 15-20% additional phosphorylation sites than control experiments without FAIMS. In comparison to liquid chromatography prefractionation, FAIMS experiments yielded similar or superior results when analyzing up to four discrete gas-phase fractions. Although using FAIMS led to a modest reduction in the precision of quantitative measurements when using label-free approaches, the data collected with FAIMS yielded a 26% increase in total reproducible measurements. Overall, we conclude that the new FAIMS technology is a valuable addition to any phosphoproteomic workflow, with greater benefits emerging from longer analyses and higher amounts of material.

Immunopharmacology and Quantitative Analysis of Tyrosine Kinase Signaling.

In this article we describe the use of pharmacological and genetic tools coupled with immunoblotting (Western blotting) and targeted mass spectrometry to quantify immune signaling and cell activation mediated by tyrosine kinases. Transfer of the ATP γ phosphate to a protein tyrosine residue activates signaling cascades regulating the differentiation, survival, and effector functions of all cells, with unique roles in immune antigen receptor, polarization, and other signaling pathways. Defining the substrates and scaffolding interactions of tyrosine kinases is critical for revealing and therapeutically manipulating mechanisms of immune regulation. Quantitative analysis of the amplitude and kinetics of these effects is becoming ever more accessible experimentally and increasingly important for predicting complex downstream effects of therapeutics and for building computational models. Secondarily, quantitative analysis is increasingly expected by reviewers and journal editors, and statistical analysis of biological replicates can bolster claims of experimental rigor and reproducibility. Here we outline methods for perturbing tyrosine kinase activity in cells and quantifying protein phosphorylation in lysates and immunoprecipitates. The immunoblotting techniques are a guide to probing the dynamics of protein abundance, protein–protein interactions, and changes in post‐translational modification. Immunoprecipitated protein complexes can also be subjected to targeted mass spectrometry to probe novel sites of modification and multiply modified or understudied proteins that cannot be resolved by immunoblotting. Together, these protocols form a framework for identifying the unique contributions of tyrosine kinases to cell activation and elucidating the mechanisms governing immune cell regulation in health and disease. © 2020 The Authors. Basic Protocol 1: Quantifying protein phosphorylation via immunoblotting and near‐infrared imaging Alternate Protocol: Visualizing immunoblots using chemiluminescence Basic Protocol 2: Enriching target proteins and isolation of protein complexes by immunoprecipitation Support Protocol: Covalent conjugation of antibodies to functionalized beads Basic Protocol 3: Quantifying proteins and post‐translational modifications by targeted mass spectrometry

Isoelectric Focusing to Quantify Rhodopsin Phosphorylation in Mouse Retina.

Rhodopsin is a G-protein coupled receptor (GPCR) that mediates vision under dim light. Upon light exposure, rhodopsin is phosphorylated at multiple serine and threonine sites at its carboxyl-terminus by rhodopsin kinase (GRK1). This, in turn, reduces its ability to activate the visual G-protein transducin. Binding of light-activated, phosphorylated rhodopsin by arrestin (ARR1) fully terminates the catalytic activity of rhodopsin. Quantification of the levels of the differentially phosphorylated rhodopsin species provides definitive information about the role of phosphorylated rhodopsin in visual functions. Isoelectric Focusing (IEF) is a technique which is used to separate ampholytic components, such as proteins, based on their isoelectric point (pI). It is a useful technique used to distinguish protein isoforms and post-translational modifications such as phosphorylation, glycosylation, deamination, and acetylation, due to their effects on the protein's pI. Isoelectric Focusing can provide high resolution of differentially phosphorylated forms of a protein. Though other techniques such as kinase activity assays, phospho-specific antibodies, western blot, enzyme-linked immunosorbent assays (ELISA), radiolabeling and mass spectrometry are used to detect and quantify protein phosphorylation, IEF is a simple and cost-effective method to quantify rhodopsin phosphorylation, as it can readily detect individual phosphorylated forms. Here we provide a detailed protocol for determining phosphorylated rhodopsin species using the Isoelectric Focusing technique.

Phospho-protein Analysis in Adherent Cells Using Flow Cytometry.

Protein phosphorylation is one of the most important post-translational modifications, which acts as a reversible on or off switch for the activity of a large number of proteins. Analyzing the phosphorylation status of different proteins can reveal the alterations in the state of the cells in response to cellular damage, cancer and pharmaceutical drugs. Techniques such as mass spectrometry, radiolabeling, 2D-gel electrophoresis and western blotting are used to quantify protein phosphorylation. These assays can quantify phosphorylation in the bulk population of cells, however, flow cytometry can couple cell surface marker expression data with phosphorylation data to understand differential signaling in a sub-population within a heterogeneous population of cells. Our protocol describes the use of flow-cytometry for rapid and single cell-based quantification of intracellular phospho-protein with the help of anti-phospho protein specific antibody.

Characterization of protein N-glycosylation by tandem mass spectrometry using complementary fragmentation techniques

The analysis of post-translational modifications (PTMs) by proteomics is regarded as a technically challenging undertaking. While in recent years approaches to examine and quantify protein phosphorylation have greatly improved, the analysis of many protein modifications, such as glycosylation, are still regarded as problematic. Limitations in the standard proteomics workflow, such as use of suboptimal peptide fragmentation methods, can significantly prevent the identification of glycopeptides. The current generation of tandem mass spectrometers has made available a variety of fragmentation options, many of which are becoming standard features on these instruments. We have used three common fragmentation techniques, namely CID, HCD, and ETD, to analyze a glycopeptide and highlight how an integrated fragmentation approach can be used to identify the modified residue and characterize the N-glycan on a peptide.

Designed phosphoprotein recognition in Escherichia coli.

Protein phosphorylation is a central biological mechanism for cellular adaptation to environmental changes. Dysregulation of phosphorylation signaling is implicated in a wide variety of diseases. Thus, the ability to detect and quantify protein phosphorylation is highly desirable for both diagnostic and research applications. Here we present a general strategy for detecting phosphopeptide–protein interactions in Escherichia coli. We first redesign a model tetratricopeptide repeat (TPR) protein to recognize phosphoserine in a sequence-specific fashion and characterize the interaction with its target phosphopeptide in vitro. We then combine in vivo site-specific incorporation of phosphoserine with split mCherry assembly to observe the designed phosphopeptide–protein interaction specificity in E. coli. This in vivo strategy for detecting and characterizing phosphopeptide–protein interactions has numerous potential applications for the study of natural interactions and the design of novel ones.

Stable Isotope Labeling of Phosphoproteins for Large-scale Phosphorylation Rate Determination

Signals that control responses to stimuli and cellular function are transmitted through the dynamic phosphorylation of thousands of proteins by protein kinases. Many techniques have been developed to study phosphorylation dynamics, including several mass spectrometry (MS)-based methods. Over the past few decades, substantial developments have been made in MS techniques for the large-scale identification of proteins and their post-translational modifications. Nevertheless, all of the current MS-based techniques for quantifying protein phosphorylation dynamics rely on the measurement of changes in peptide abundance levels, and many methods suffer from low confidence in phosphopeptide identification due to poor fragmentation. Here we have optimized an approach for the stable isotope labeling of amino acids by phosphate using [γ-¹⁸O₄]ATP in nucleo to determine global site-specific phosphorylation rates. The advantages of this metabolic labeling technique are increased confidence in phosphorylated peptide identification, direct labeling of phosphorylation sites, measurement phosphorylation rates, and the identification of actively phosphorylated sites in a cell-like environment. In this study we calculated approximate rate constants for over 1,000 phosphorylation sites based on labeling progress curves. We measured a wide range of phosphorylation rate constants from 0.34 min⁻¹ to 0.001 min⁻¹. Finally, we applied stable isotope labeling of amino acids by phosphate to identify sites that have different phosphorylation kinetics during G1/S and M phase. We found that most sites had very similar phosphorylation rates under both conditions; however, a small subset of sites on proteins involved in the mitotic spindle were more actively phosphorylated during M phase, whereas proteins involved in DNA replication and transcription were more actively phosphorylated during G1/S phase. The data have been deposited to the ProteomeXchange with the identifier PXD000680.

Protein Phosphorylation Profiling Using an In Situ Proximity Ligation Assay: Phosphorylation of AURKA-Elicited EGFR-Thr654 and EGFR-Ser1046 in Lung Cancer Cells

The epidermal growth factor receptor (EGFR), which is up-regulated in lung cancer, involves the activation of mitogenic signals and triggers multiple signaling cascades. To dissect these EGFR cascades, we used 14 different phospho-EGFR antibodies to quantify protein phosphorylation using an in situ proximity ligation assay (in situ PLA). Phosphorylation at EGFR-Thr654 and -Ser1046 was EGF-dependent in the wild-type (WT) receptor but EGF-independent in a cell line carrying the EGFR-L858R mutation. Using a ProtoAarray™ containing ∼5000 recombinant proteins on the protein chip, we found that AURKA interacted with the EGFR-L861Q mutant. Moreover, overexpression of EGFR could form a complex with AURKA, and the inhibitors of AURKA and EGFR decreased EGFR-Thr654 and -Ser1046 phosphorylation. Immunohistochemical staining of stage I lung adenocarcinoma tissues demonstrated a positive correlation between AURKA expression and phosphorylation of EGFR at Thr654 and Ser1046 in EGFR-mutant specimens, but not in EGFR-WT specimens. The interplay between EGFR and AURKA provides an explanation for the difference in EGF dependency between EGFR-WT and EGFR-mutant cells and may provide a new therapeutic strategy for lung cancer patients carrying EGFR mutations.

A Robust Error Model for iTRAQ Quantification Reveals Divergent Signaling between Oncogenic FLT3 Mutants in Acute Myeloid Leukemia

The FLT3 receptor tyrosine kinase plays an important role in normal hematopoietic development and leukemogenesis. Point mutations within the activation loop and in-frame tandem duplications of the juxtamembrane domain represent the most frequent molecular abnormalities observed in acute myeloid leukemia. Interestingly these gain-of-function mutations correlate with different clinical outcomes, suggesting that signals from constitutive FLT3 mutants activate different downstream targets. In principle, mass spectrometry offers a powerful means to quantify protein phosphorylation and identify signaling events associated with constitutively active kinases or other oncogenic events. However, regulation of individual phosphorylation sites presents a challenging case for proteomics studies whereby quantification is based on individual peptides rather than an average across different peptides derived from the same protein. Here we describe a robust experimental framework and associated error model for iTRAQ-based quantification on an Orbitrap mass spectrometer that relates variance of peptide ratios to mass spectral peak height and provides for assignment of p value, q value, and confidence interval to every peptide identification, all based on routine measurements, obviating the need for detailed characterization of individual ion peaks. Moreover, we demonstrate that our model is stable over time and can be applied in a manner directly analogous to ubiquitously used external mass calibration routines. Application of our error model to quantitative proteomics data for FLT3 signaling provides evidence that phosphorylation of tyrosine phosphatase SHP1 abrogates the transformative potential, but not overall kinase activity, of FLT3-D835Y in acute myeloid leukemia.

Quantitation of protein phosphorylation in pregnant rat uteri using stable isotope dimethyl labeling coupled with IMAC

Quantitative analysis of protein phosphorylation provides important insights into molecular signaling mechanisms and a better understanding of many cellular processes. In this study, we coupled stable isotope dimethyl labeling with immobilized metal affinity chromatography (IMAC) enrichment to quantify protein phosphorylation at MS-determined phosphorylation sites. The proposed method was first characterized using alpha- and beta-casein as two model phosphoproteins, and further applied to the analysis of pregnant rat uteri with and without treatment with 8-bromo-cGMP. Dimethyl labeling has several significant advantages: global, fast (within 5 min) and complete (near 100%). Our results indicate that the labeling has no adverse effect on the IMAC enrichment for tryptic peptides having single and multiple phosphorylation sites. Moreover, the enhanced a1 signal and the complete reaction by dimethyl labeling provide unequivocal identification of both the N-terminal amino acid and the number of the labeling site. Using these two criteria in data validation, which is particularly important for identifying phosphoproteins, we found that the confidence in interpreting dimethyl-labeled peptides had greatly increased. In the analysis of late gestation rat uteri, the abundance ratio between treated and un-treated phosphopeptide signals ranged from 0.51 to 1.69 with an average of around 1.01 +/- 0.25. The obtained ratio of the phosphorylation levels at Ser 15 of HSP27 was further confirmed by the consistent results obtained from Western blot analyses. Based on the analysis of the results, it is interesting to note that the activated cGMP dependent protein kinase G (PKG) seems to affect the phosphorylation of proteins associated with the inhibition of cell migration and proliferation, redistribution of actin-associated proteins, and the increase of protein synthesis in late-gestation uteri. These observations provide important evidence suggesting that activated PKG may play a critical role in the shift of pregnant uteri from proliferative to hypertrophic states.