Hydrogen Deuterium Exchange (HDX) Mass Spectrometry (MS) is a sensitive analytical technique that provides information on protein conformation and dynamics in solution. It is commonly used in the study of protein-ligand and protein-protein interactions and more recently in the pharmaceutical industry for epitope mapping, screening drug candidates and in the comparison of biopharmaceuticals to biosimilars. HDX-MS monitors the exchange of protein backbone hydrogen atoms with deuterium in solution. Recent advancements in HDX automation and data analysis, have taken the emphasis off developing a fundamental understanding of HDX, which is still lacking. This tutorial review will cover the different mechanisms of exchange and how the exchange reaction is affected by various factors. We also explore the basis of data analysis and the difficulties that often arise in the interpretation of site-specific and segment-averaged HDX data, such as overlapping isotopic distributions and correct identification of peptides. Initial data analysis generates a list of peptides and the deuterium incorporation of each peptide at each labeling time point, i.e., a set of deuterium uptake profiles. Data interpretation and error analysis is subsequently required to ensure that deuterium uptake profiles accurately reflect conformational dynamics in solution. Finally, this review will also discuss the different ways in which HDX data can be represented and how the data can be interpreted.

Conformational dynamics play a critical role in ligand binding, often conferring divergent activities and specificities even in species with highly similar ground-state structures. Here, we employ time-resolved electrospray ionization hydrogen-deuterium exchange (TRESI-HDX) to characterize the changes in dynamics that accompany oligonucleotide binding in the atypical RNA recognition motif (RRM2) in the C-terminal domain (CTD) of human La protein. Using this approach, which is uniquely capable of probing changes in the structure and dynamics of weakly ordered regions of proteins, we reveal that binding of RRM2 to a model 23-mer single-stranded RNA and binding of RRM2 to structured IRES domain IV of the hepatitis C viral (HCV) RNA are driven by fundamentally different dynamic processes. In particular, binding of the single-stranded RNA induces helical "unwinding" in a region of the CTD previously hypothesized to play an important role in La and La-related protein-associated RNA remodeling, while the same region becomes less dynamic upon engagement with the double-stranded HCV RNA. Binding of double-stranded RNA also involves less penetration into the RRM2 binding pocket and more engagement with the unstructured C-terminus of the La CTD. The complementarity between TRESI-HDX and Δδ nuclear magnetic resonance measurements for ligand binding analysis is also explored.

Intrinsically disordered proteins (IDPs) have long been a challenge to structural biologists due to their lack of stable secondary structure elements. Hydrogen-Deuterium Exchange (HDX) measured at rapid time scales is uniquely suited to detect structures and hydrogen bonding networks that are briefly populated, allowing for the characterization of transient conformers in native ensembles. Coupling of HDX to mass spectrometry offers several key advantages, including high sensitivity, low sample consumption and no restriction on protein size. This technique has advanced greatly in the last several decades, including the ability to monitor HDX labeling times on the millisecond time scale. In addition, by incorporating the HDX workflow onto a microfluidic platform housing an acidic protease microreactor, we are able to localize dynamic properties at the peptide level. In this study, Time-Resolved ElectroSpray Ionization Mass Spectrometry (TRESI-MS) coupled to HDX was used to provide a detailed picture of residual structure in the tau protein, as well as the conformational shifts induced upon hyperphosphorylation.

The ongoing shift from small molecule drugs to protein therapeutics in the pharmaceuticals industry presents a considerable challenge to generic drug developers who are increasingly required to demonstrate biosimilarity for biological macromolecules, a task that is decidedly more complex than doing the same for small molecule drugs. In this work, we demonstrate a multipronged mass‐spectrometry‐based workflow that allows rapid and facile molecular characterization of antibody‐based protein therapeutics, applied to biosimilars development. Specifically, we use a combination of native mass spectrometry (MS), ion mobility spectrometry (IMS), and global time‐resolved hydrogen deuterium exchange (HDX) to provide an unambiguous assessment of the structural, dynamic, and chemical similarity between Avastin (bevacizumab) and a biosimilar in the late stages of pre‐clinical development. Minor structural and dynamic differences between the biosimilar and Avastin, and between lots of the biosimilar, were tested for functional relevance using Surface Plasmon Resonance‐derived kinetic and equilibrium binding parameters.

The success of bevacizumab (Avastin), a monoclonal antibody (mAb) anticancer drug targeting vascular endothelial growth factor A (VEGF-A), has motivated the development of biosimilars. Establishing target epitope similarity using epitope mapping is a critical step in preclinical mAb biosimilar development. Here we use time-resolved electrospray ionization hydrogen− deuterium exchange (HDX) mass spectrometry to rapidly compare the epitopes of commercial Avastin and a biosimilar in preclinical development (ApoBev) on an extended construct of VEGF-A. The Avastin and ApoBev epitopes determined in our experiments agree with each other and with the known epitope derived from the Avastin Fab domain/truncated VEGF co-crystal structure. However, subtly different allosteric effects observed exclusively at short (millisecond) HDX labeling times may reflect a slightly different binding mode for ApoBev.