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Production, extraction, purification, and stabilization of integral membrane proteins are key steps for successful structural biology studies, in particular for X-ray crystallography or single particle microscopy. Here, we present the purification protocol of CntI from Pseudomonas aeruginosa, a new metallophore exporter of the Drug Metabolite Transporter (DMT) family involved in pseudopaline secretion. Subsequent to CntI purification, we optimized the buffer pH, salts, and additives by differential scanning fluorimetry (DSF), also known as Thermofluor Assay (TFA) or fluorescent thermal stability assay (FTSA), with the use of dye 1-AnilinoNaphthalene-8-Sulfonic acid (ANS), a fluorescent molecule compatible with detergents. After the buffer optimization, the purified CntI was analyzed by Size Exclusion Chromatography coupled with Multi-Angle Laser Light Scattering (SEC-MALLS), UV absorbance, and Refractive Index detectors, in order to determine the absolute molar mass of the protein-detergent complex, the detergent amount bound to the protein and the amount of protein-free detergent micelles. Altogether, these biophysical techniques give preliminary and mandatory information about the suitability of the purified membrane protein for further biophysical or structural investigations., (© 2024. The Author(s), under exclusive license to Springer Science+Business Media, LLC, part of Springer Nature.)

Membrane proteins are responsible for a large variety of tasks in organisms and of particular interesting as drug targets. At the same time, they are notoriously difficult to work with and require a thorough characterization before proceeding with structural studies. Here, we present a biophysical pipeline to characterize membrane proteins focusing on the optimization of stability, aggregation behavior, and homogeneity. The pipeline shown here is built on three biophysical techniques: differential scanning fluorimetry using native protein fluorescence (nano differential scanning fluorimetry), dynamic light scattering, and mass photometry. For each of these techniques, we provide detailed protocols for performing experiments and data analysis., (© 2023. The Author(s), under exclusive license to Springer Science+Business Media, LLC, part of Springer Nature.)

Thermofluor is a fluorescence-based thermal shift assay, which measures temperature-induced protein unfolding and thereby yields valuable information about the integrity of a purified recombinant protein. Analysis of ligand binding to a protein is another popular application of this assay. Thermofluor requires neither protein labeling nor highly specialized equipment, and can be performed in a regular real-time PCR instrument. Thus, for a typical molecular biology laboratory, Thermofluor is a convenient method for the routine assessment of protein quality. Here, we provide Thermofluor protocols using the example of Cdc123. This ATP-grasp protein is an essential assembly chaperone of the eukaryotic translation initiation factor eIF2. We also report on a destabilized mutant protein version and on the ATP-mediated thermal stabilization of wild-type Cdc123 illustrating protein integrity assessment and ligand binding analysis as two major applications of the Thermofluor assay., (© 2022. The Author(s).)

Nano differential scanning fluorimetry is used to quantify protein thermostability and has substantially expanded the spectrum of convenient biophysical parameters used to characterize proteins. Here, this technique is used to measure the ΔT m shift for single-domain antibodies (sdAbs), which represents a comprehensive metric for the aggregation propensity of sdAbs upon heat-denaturation. By relating two melting curves at different protein concentrations, the ΔT m shift described in this protocol is ideally suited for high-throughput measurements to guide protein engineering, formulation development, and developability assessment of sdAbs., (© 2022. The Author(s), under exclusive license to Springer Science+Business Media, LLC, part of Springer Nature.)

A thermal shift assay (TSA) involves measuring the effect of a compound on the thermal stability of a protein as an indirect measure of ligand binding. In this chapter, we provide a protocol for a conventional TSA with recombinant/purified proteins using differential scanning fluorimetry (DSF), followed by a protocol for a Cellular Thermal Shift Assay (CETSA ® ), which measures the soluble cellular protein remaining after a transient heat shock of live cells to detect intracellular ligand binding.

Thermofluor or thermal shift assay is an easily implementable, high-throughput method for assessing the thermostability of proteins and the influence of various ligands on that stability. It is particularly useful for the assaying of ligands that may stabilize oligomeric helicases, which rely on both substrates (oligonucleotides) and nucleotide cofactors (ATP analogues) for their stability in a functional state. In this chapter, we describe the rationale and present a basic protocol for the use of this technique. Multi-ligand screening is also discussed via a worked example of the stabilization of a hexameric RNA helicase, a target protein for structural studies in our laboratories.

Synthetic analogs of the second transmembrane domain (TM) containing a portion of the extracellular loop 1 of G-protein-coupled receptors (GPCR) can serve as biased antagonists of the corresponding receptor. Analogs with negative charges added to the extracellular end self-assemble into round structures. Addition of polyethylene glycol chains of defined length to the C-terminus of the peptides prevents super aggregation and results in highly uniform particles that can fuse with cell membranes spontaneously. Added PEG chains slow down cell fusion, while attachment of receptor ligands to the surface of particles results in receptor-mediated membrane fusion and cell-selective delivery. Critical assembly concentration of TM peptide particles is in the nanomolar range and thus requires nontraditional methods of determination. In this chapter, we outline sequence selection and design of self-assembling GPCR antagonists, methods of the preparation of the nanoparticles, and biophysical methods of particle characterization. The protocols allow for straightforward rational design, generation, and characterization of self-assembling GPCR antagonists for a variety of applications.

Differential scanning fluorimetry (DSF) can be used to detect the binding of a small molecule ligand to a purified target protein. Upon binding with certain ligands, the protein can be stabilized from thermal denaturation. DSF uses a fluorescent dye and Real-Time PCR instrument to detect the unfolding process of proteins during thermal denaturation. The experiment can be set up and finished in 1 day once the purified protein is available.

Despite the discovery of protein histidine (His) phosphorylation nearly six decades ago, difficulties in measuring and quantifying this unstable post-translational modification (PTM) have limited its mechanistic analysis in prokaryotic and eukaryotic signaling. Here, we describe reliable procedures for affinity purification, cofactor-binding analysis and antibody-based detection of phosphohistidine (pHis), on the putative human His kinases NME1 (NDPK-A) and NME2 (NDPK-B) and the glycolytic phosphoglycerate mutase PGAM1. By exploiting isomer-specific monoclonal N1-pHis and N3-pHis antibodies, we describe robust protocols for immunological detection and isomer discrimination of site-specific pHis, including N3-pHis on His 11 of PGAM1.

Systematic identification of buffer formulations and small molecule chaperones that improve the expression, stability, and storage of proteins with therapeutic interest has gained enormous importance in biochemical research as well as in biotechnology and biomedical applications. In particular, the biochemical characterization of disease-related proteins and their genetic variants that result in misfolding requires systematic determination of protein stability, screening of optimal buffer conditions for biophysical and structural studies, and in some cases, the identification of small molecule chaperones with the potential to ameliorate folding defects. Among the several techniques available, differential scanning fluorimetry (DSF) is currently an extensively employed screening and analysis method for thermal shift and protein stability assays. Here we describe a step-by-step generic protocol for fast characterization of protein thermal stability and analysis of stabilization in thermal-shift assays by additives, ligands and chemical chaperones using β-oxidation mitochondrial dehydrogenases as model. These enzymes are associated to inborn errors of metabolism caused by mutant variants with folding and stability defects for which we previously established folding correction afforded by their cognate cofactors and substrates. With this example we thus illustrate the potential applications of the method in screening small molecule folding correctors among metabolites, ligands, cofactors or candidate drugs with therapeutic potential in protein folding diseases.

The majority of bacterial chemoreceptors remain functionally un-annotated. The knowledge of chemoreceptor function, however, is indispensable to understanding the evolution of the chemotaxis system in bacteria with different lifestyles. Significant progress in the annotation of chemoreceptor function has been made using experimental strategies that are based on the individual, genetically engineered ligand binding domain (LBD) of chemoreceptors. There is now evidence that all major classes of LBDs can be produced as individual domains that retain their ligand binding activity. Here, we provide a protocol for the combined use of high-throughput ligand screening using Differential Scanning Fluorimetry followed by Isothermal Titration Calorimetry to identify and characterize ligands that bind to recombinant chemoreceptor LBDs. This approach has been shown to be very efficient for determining the function of novel chemoreceptors.

Employing biophysical and structural methods is a powerful way to elucidate mechanisms of molecular recognition in bacterial pathogenesis. Such studies invariably depend on the production of pure, folded and stable proteins. Many proteins that can be expressed recombinantly ultimately fail to meet one or more of these criteria. The cag proteins from Helicobacter pylori form a secretion system that delivers the oncoprotein, CagA, into human gastric epithelial cells through an interaction between CagL and host cell integrins, where it can cause gastric adenocarcinoma. Expression of full length CagA and CagL is problematic as CagA undergoes rapid degradation during purification and CagL is thermally unstable. Here, we describe a method for the purification of CagA that results in the production of the full length protein through coexpression with its endogenous chaperone, CagF, and its subsequent separation from its chaperone. Furthermore, we detail the production of CagL and the use of differential scanning fluorimetry to identify how CagL is thermally stabilized by reduced pH, which led to a new crystal form of CagL and novel insight to pathogenic mechanisms. The methods described here for the production of stable cag proteins can be applied to a wide range of proteins involved in bacterial pathogenesis.