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CoSAXS is a state-of-the-art SAXS/WAXS beamline exploiting the high brilliance of the MAX IV 3 GeV synchrotron. By coupling advances in sample environment control with fast X-ray detectors, millisecond time-resolved scattering methods can follow structural dynamics of proteins in solution. In the present work, four sample environments are discussed. A sample environment for combined SAXS with UV-vis and fluorescence spectroscopy (SUrF) enables a comprehensive understanding of the time evolution of conformation in a model protein upon acid-driven denaturation. The use of microfluidic chips with SAXS allows the mapping of concentration with very small sample volumes. For highly reproducible sequences of mixing of components, it is possible using stopped-flow and SAXS to access the initial effects of mixing at 2 millisecond timescales with good signal to noise to allow structural interpretation. The intermediate structures in a protein are explored under light and temperature perturbations by using lasers to "pump" the protein and SAXS as the "probe". The methods described demonstrate that features at low q, corresponding to cooperative motions of the atoms in a protein, could be extracted at millisecond timescales, which results from CoSAXS being a highly-stable, low background, dedicated SAXS beamline., (Copyright © 2024. Published by Elsevier Inc.)

S-adenosylmethionine (SAM) is most widely known as the biological methylating agent of methyltransferases and for generation of radicals by the iron-sulfur dependent Radical SAM enzymes. SAM also serves as a substrate in biosynthetic reactions that harvest the aminobutyrate moiety of the methionine, producing methylthioadenosine as a co-product. These reactions are found in the production of polyamines such as spermine, siderophores derived from nicotianamine, and opine metallophores staphylopine and pseudopaline, among others. This procedure defines a highly sensitive, continuous fluorescence assay for the determination of steady state kinetic parameters for enzymes that generate the co-product methylthioadenosine., (Copyright © 2024. Published by Elsevier Inc.)

Biophysical coupling between the inner and outer leaflets, known as inter-leaflet or transbilayer coupling, is a fundamental organizational principle in the plasma membranes of live mammalian cells. Lipid-based interactions between the two leaflets are proposed to be a primary mechanism underlying transbilayer coupling. However, there are only a few experimental evidence supporting the existence of such interactions in live cells. This is seemingly due to the lack of experimental strategies to perturb the lipid composition in one leaflet and quantitative techniques to evaluate the biophysical properties of the opposite leaflet. The existing strategies often dependent on immobilization and clustering a component in one of the leaflets and technically demanding biophysical tools to evaluate the effects on the opposing leaflet. In the recent years, the London group developed a simple but elegant method, namely methyl-alpha-cyclodextrin catalyzed lipid exchange (LEX), to efficiently exchange outer leaflet lipids with an exogenous lipid of choice. Here, we adopted this method to perturb outer leaflet lipid composition. The corresponding changes in the inner leaflet is evaluated by comparing the diffusion of lipid probes localized in this leaflet in unperturbed and perturbed conditions. We employed highly multiplexed imaging fluorescence correlation spectroscopy (ImFCS), realized in a commercially available or home-built total internal reflection fluorescence microsocope equipped with a fast and sensitive camera, to determine diffusion coefficient of the lipid probes. Using the combination of LEX and ImFCS, we directly demonstrate lipid-based transbilayer coupling that does not require immobilization of membrane components in live mast cells in resting conditions. Overall, we present a relatively straightforward experimental strategy to evaluate transbilayer coupling quantitively in live cells., (Copyright © 2024. Published by Elsevier Inc.)

Hyperspectral imaging is a technique that captures a three-dimensional array of spectral information at each spatial location within a sample, enabling precise characterization and discrimination of biological structures, materials, and chemicals, based on their unique spectral features. Nowadays most commercially available confocal microscopes allow hyperspectral imaging measurements, providing a valuable source of spatially resolved spectroscopic data. Spectral phasor analysis quantitatively and graphically transforms the fluorescence spectra at each pixel of a hyperspectral image into points in a polar plot, offering a visual representation of the spectral characteristics of fluorophores within the sample. Combining the use of environmentally sensitive dyes with phasor analysis of hyperspectral images provides a powerful tool for measuring small changes in lateral membrane heterogeneity. Here, we focus on applications of spectral phasor analysis for the probe LAURDAN on model membranes to resolve packing and hydration. The method is broadly applicable to other dyes and to complex systems such as cell membranes., (Copyright © 2024. Published by Elsevier Inc.)

RNA targeted high-throughput assays that allow for rapid detection of high affinity binding ligands are important in RNA recognition studies. A number for fluorescent dyes have been reported that can assist in rapidly identifying nucleic acid (RNA) binding elements without the need for immobilization of RNA or the ligand. A number of these dyes are planar aromatic molecules that bind non-specifically to nucleic acids and often distort their parent nucleic acid structures leading to ambiguity in the interpretation of results. In this light, we report here, the use of an aminoglycoside (neomycin) based fluorescent probe (F-Neo) which can reversibly bind to different RNA motifs and help identify ligands with needed affinity and selectivity, without any immobilization of the probe or the target. In this chapter, we provide the details of the assay development, experimental considerations and data analysis to use the probe and identify novel ligands. We then provide a brief introduction to calorimetry (ITC) and circular dichroism (CD) spectroscopy based methods in validating the binding of such identified compounds., (© 2019 Elsevier Inc. All rights reserved.)

Cellular functions are often controlled by small molecular weight molecules such as metabolites. Microorganisms, mainly prokaryotes, have evolved sensing and regulatory mechanisms based on transcriptional regulators (TRs) that are able to activate gene expression in response to changes in intra- and extracellular metabolite (ligand) concentrations. To understanding control mechanisms and cell factory development in synthetic biology applications, high throughput analytical procedures are required. In this chapter, we outline a methodological pipeline to design and build reporter constructs enabling the characterization of metabolite-responsive inducible gene expression systems. As an example, we present the design, cloning and characterization of the itaconate-inducible system which is composed of the LysR-type transcriptional regulator ItcR and the promoter P ccl from Yersinia pseudotuberculosis. Fluorescence-based plate reader and flow cytometry assays are described and the steps for performing data analysis are provided., (© 2019 Elsevier Inc. All rights reserved.)

Protein phosphatases act in concert with protein kinases to regulate and maintain the phosphoproteome. However, the catalog of chemical tools to directly monitor the enzymatic activity of phosphatases has lagged behind their kinase counterparts. In this chapter, we provide protocols for repurposing the phosphorylation-sensitive sulfonamido-oxine fluorophore known as Sox to afford direct activity probes for phosphatases. With validated activity probes in-hand, inhibitor screens can be conducted with recombinant enzyme and the role of phosphatases in cell signaling can be investigated in unfractionated cell lysates., (© 2019 Elsevier Inc. All rights reserved.)

Understanding how to design small molecules that target coding and non-coding RNA has the potential to exponentially increase the number of therapeutically-relevant druggable targets, which are currently mostly proteins. However, there is limited information on the principles at the basis of RNA recognition. In this chapter, we describe a pattern-based technique that can be used for the simultaneous elucidation of RNA motifs and small molecule features for RNA selective recognition, termed Pattern Recognition of RNA by Small Molecules (PRRSM). We provide protocols for the computational design and synthetic preparation of an RNA training set as well as how to perform the assay in plate reader format. Furthermore, we provide details on how to perform and interpret the statistical analysis and indicate possible future extensions of the technique. By combining insights into characteristics of the small molecules and of the RNA that leads to differentiation, PRRSM promises to accelerate the elucidation of the determinants at the basis of RNA recognition., (© 2019 Elsevier Inc. All rights reserved.)

Glucocerebrosidase (GCase) is a lysosomal glycoside hydrolase that cleaves the glycolipid glucosylceramide (GlcCer). Deficiencies of this enzyme lead to accumulation of GlcCer and the development of the lysosomal storage disease known as Gaucher's disease. Recently, loss-of-function mutations in the GBA1 gene that encodes GCase have been linked to Parkinson's disease. Currently pursued therapeutic strategies to increase GCase involve enzyme replacement therapy, chemical chaperone therapy, and GCase activators. A challenge associated with advancing such strategies is to efficiently monitor GCase activity within the lysosomes of live cells. In this chapter, we review the design and use of the fluorescent-quenched probe GBA1-FQ2 to quantitatively measure GCase activity in lysosomes of live cells., (© 2018 Elsevier Inc. All rights reserved.)

Intrinsically disordered proteins are abundant in signaling processes such as transcription. Suitable binding and unbinding rates of proteins with their partners are critical for allowing them to perform their biological roles. Understanding how these are achieved, and indeed designing strategies for intervening or modulating related biological processes, therefore requires kinetic studies. In this chapter, we describe stopped-flow-based methods for determining association and dissociation rate constants for pairs of macromolecular binding partners. We describe how to select the simplest appropriate model to describe the interaction, and highlight cases where it is possible to distinguish between induced fit and conformational selection binding mechanisms. Finally, we go on to describe methods for examining the role of electrostatic forces in binding processes, and for describing the transition state for binding processes that have folding associated with them., (© 2018 Elsevier Inc. All rights reserved.)

Fluorescence correlation spectroscopy (FCS) is a single-molecule sensitive technique with widespread applications in biophysics. However, conventional microscope-based FCS setups have limitations in performing certain experiments such as those requiring agitations such as stirring or heating, and those involving measurements in solvents with the mismatch of refractive indices. We have recently developed an FCS setup that is suitable for performing measurements inside regular cuvettes. The cuvette-FCS is suitable for performing single-molecule measurements in experiments that are regularly performed in spectrofluorometers but are generally avoided in microscope-based FCS. Here we describe building and characterization of the performance of the cuvette-FCS setup in detail. Finally, we have used a natively folded protein and an intrinsically disordered protein to demonstrate and describe how cuvette-FCS can be applied conveniently to measure urea-dependent expansion of hydrodynamic size of proteins., (© 2018 Elsevier Inc. All rights reserved.)

Intrinsically disordered proteins (IDPs) comprise a large fraction of eukaryotic proteomes. IDPs are prevalent in cellular regulation, signaling networks, and disease pathways. The abundance and activity of IDPs is tightly controlled at multiple levels, and their dysregulation is associated with disease. Because of the importance of IDPs in both normal and disease states of the cell, IDPs are attractive targets for modulation by small molecules both to understand their biology and to provide potential drug leads. Multiple screens have successfully identified small molecules that bind to IDPs. Here, we describe how surface plasmon resonance, NMR, and fluorescence methods can be used to characterize the direct binding affinity between small molecules and IDPs. We describe how these techniques can contribute to identifying previously unknown small-molecule binding sites on IDPs., (© 2018 Elsevier Inc. All rights reserved.)

Intrinsically disordered proteins (IDPs) and regions (IDRs) make up a significant part of the proteome and facilitate a wide range of physiological and pathological functions that are only beginning to be understood. As such, they are highly attractive targets for drug development and bioengineering. However, their inability to adopt well-defined structures provides significant obstacles for developing ligands that regulate their behaviors. In this chapter, we review how the conformational flexibility of IDPs and their propensity to phase separate make them tractable targets for small-molecule manipulation. We also describe both theoretical and experimental approaches to characterize disordered proteins, including novel thermodynamic and single-molecule techniques that help identify complimentary partners of IDPs and their ability to shift protein ensembles toward preferred conformations., (© 2018 Elsevier Inc. All rights reserved.)

Nucleotide hydrolases play integral yet poorly understood roles in several metallocluster biosynthetic pathways. For example, the cytosolic iron-sulfur cluster assembly (CIA) is initiated by the CIA scaffold, an ATPase which builds new iron-sulfur clusters for proteins localized to the cytosol and the nucleus in eukaryotic organisms. While in vivo studies have demonstrated the scaffold's nucleotide hydrolase domain is vital for its function, in vitro approaches have not revealed tight allosteric coupling between the cluster scaffolding site and the ATPase site. Thus, the role of ATP hydrolysis has been hard to pinpoint. Herein, we describe methods to probe the nucleotide affinity and hydrolysis activity of the CIA scaffold from yeast, which is comprised of two homologous polypeptides called Nbp35 and Cfd1. In particular, we report two different equilibrium binding assays that make use of commercially available fluorescent nucleotide analogs. Importantly, these assays can be applied to probe nucleotide affinity of both the apo- and holo-forms of the CIA scaffold. Generally, these fluorescent nucleotide analogs have been underutilized to probe metal trafficking NTPase because one of the most commonly used probes, mantATP, which is labeled with the methylanthraniloyl probe via the 2' or 3' sugar hydroxyls, has an absorption which overlaps with the UV-Vis features of many metal-binding proteins. However, by exploiting analogs like BODIPY-FL and trinitrophenyl-labeled nucleotides which have better photophysical properties for metalloprotein applications, these approaches have the potential to reveal the mechanistic underpinnings of NTPases required for metallocluster biosynthesis., (© 2018 Elsevier Inc. All rights reserved.)

An increasing number of intracellular and extracellular proteins are shown to interact with membrane lipids under physiological conditions. For rapid and robust quantitative measurement of lipid-protein interaction, we developed a sensitive fluorescence quenching-based assay that is universally applicable to all proteins and lipids. The assay employs fluorescence protein (FP)-tagged proteins whose fluorescence emission intensity is decreased when they bind vesicles containing quenching lipids. This simple assay can be performed with a fluorescence plate reader or a spectrofluorometer and optimized for different proteins with various combinations of FPs and quenching lipids. The assay allows a rapid, sensitive, and accurate determination of lipid specificity and affinity for various lipid-binding proteins, and high-throughput screening of molecules that modulate their membrane binding., (© 2017 Elsevier Inc. All rights reserved.)

Protein-based fluorescent biosensors are powerful tools for quantitative detection of biomolecules or drugs with high sensitivity under physiological conditions. However, conventional methods for construction of biosensors require structural data with high resolution or amino acid sequence information in most cases, which hampers applicability of this method to structurally complicated receptor proteins. To sidestep such limitations, we recently developed a new method that employs ligand-directed chemistry coupled with a bimolecular fluorescence quenching and recovery system, which enabled the conversion of various kinds of membrane-bound receptors to "turn-on" type fluorescent sensors. Here, we describe a protocol for construction of "turn-on" type fluorescent biosensors based on the GABA A receptor which permits quantitative analysis of the ligand affinity., (© 2017 Elsevier Inc. All rights reserved.)

Fluorescent proteins of different colors are useful probes to study protein structure and function, and to investigate cellular events and conditions. Large efforts have focused on engineering new properties into fluorescent proteins via rational design and directed evolution. In addition to applications in imaging of protein expression level and subcellular localization, fluorescent proteins have been increasingly engineered to act as biosensors to track concentrations of small-molecule metabolites, enzyme activities, and protein conformational changes in living cells. Unlike small-molecule fluorescence biosensors, fluorescent proteins are genetically encodable, and thus can be expressed inside living cells. Attachment of organelle-specific signals to the proteins allows their localization to be specified. Recently, a new class of fluorescent protein biosensors has been developed to include unnatural amino acids as the sensing element. The unique chemical and physical properties of the unnatural amino acids enable sensor designs that cannot be realized by using the standard genetic code with the 20 canonical amino acids. In this chapter, we detail the general procedure for the genetic incorporation of unnatural amino acids. We further present two protocols for the in vitro and in vivo detection of hydrogen peroxide (H 2 O 2 ) using a fluorescent protein biosensor that contains an unnatural amino acid, p-boronophenylalanine., (© 2017 Elsevier Inc. All rights reserved.)

Over the last few decades the development of new technologies, the fabrication of new materials, and the introduction of nanotechnologies created new trends in a series of advances that produced innovations in biological sensing devices with a wide range of application from health, security, defense, food, and medicine, to the environment. Specificity, low cost, rapidity, sensitivity, and multiplicity are some of the reasons for their growth, and their commercial success is expected to increase in the next future. Biosensors are devices in which the recognition part of the target molecule is accomplished by biological macromolecules such as proteins, enzymes, antibodies, aptamers, etc. These biomolecules are able to bind to the target molecules with high selectivity and specificity. The interaction between the target molecule and the specific biomolecule is reflected as a change of the biomolecule structural features. The extent of this change is strictly related to the biosensor response. Fluorescence spectroscopy, due to its sensitivity, is often used as the principal technique to monitor biological interactions, and thus the biosensor response as well. Both the intrinsic ultraviolet fluorescence of protein, arising from aromatic amino acids (tryptophan, tyrosine, and phenylalanine), and extrinsic fluorescent labels emitting in the visible region of the spectrum together allow for very flexible transduction of the analyte recognition, suitable for many different applications. This chapter focuses special attention on enzymes as practically unmatched recognition elements for biosensors and emphasizes the potential advantages of customized biosensor devices using apo- or holo forms of enzymes also isolated from thermophile sources., (© 2017 Elsevier Inc. All rights reserved.)

Fluorescence-based biosensors have shown themselves to be a powerful tool for the study of a variety of chemical species in biological systems, notably including metal ions. This chapter provides an overview of several important issues in using such sensors to study metallobiochemistry. These issues include selectivity for the analyte over potential interferents, including those that do not themselves induce a signal, the different forms in which metal ions are found (speciation), the utility of metal ion buffers, and the importance of kinetics in studying metal ion binding reactions. Finally, the chapter briefly discusses some of the issues in understanding whole-organism distribution of metal ions and its control., (© 2017 Elsevier Inc. All rights reserved.)

Cdc42 is a small guanosine triphosphatase (GTPase) that plays a central role in polarity development in diverse cell types. Since the activity of Cdc42 is dynamically controlled in time and space, it is required to develop a biosensor to monitor its activation in vivo. In this chapter, we describe the construction and usage of a simple and robust biosensor for monitoring active Cdc42 in budding yeast. This affinity-based biosensor uses a red fluorescent protein fused to a Cdc42- and Rac-interactive binding motif from one of the Cdc42 effector proteins. Because it binds specifically to the GTP-bound Cdc42, this biosensor can be used to monitor Cdc42 activation in vivo. This or similar biosensors can be widely used for studying GTPase signaling in other cell types because of the conserved CRIB motif present among GTPase targets., (© 2017 Elsevier Inc. All rights reserved.)

Enzymes that modify nucleobases in double-stranded genomic DNA, either as part of a DNA repair pathway or as an epigenetic modifying pathway, adopt a multistep pathway to locate target sites and reconfigure the DNA to gain access. Work on several different enzymes has shown that in almost all cases base flipping, also known as nucleotide flipping, is a key feature of specific site recognition. In this chapter, we discuss some of the strategies that can be used to perform a kinetic characterization for DNA binding and nucleotide flipping. The resulting kinetic and thermodynamic framework provides a platform for understanding substrate specificity, mechanisms of inhibition, and the roles of important amino acids. We use a human DNA repair glycosylase called alkyladenine DNA glycosylase as a case study, because this is one of the best-characterized nucleotide-flipping enzymes. However, the approaches that are described can be readily adapted to study other enzymes, and future studies are needed to understand the mechanism of substrate recognition in each individual case. As more enzymes are characterized, we can hope to uncover which features of DNA searching and nucleotide flipping are fundamental features shared by many different families of DNA modifying enzymes, and which features are specific to a particular enzyme. Such an understanding provides reasonable models for less characterized enzymes that are important for epigenetic DNA modification and DNA repair pathways., (© 2017 Elsevier Inc. All rights reserved.)

Much is known about vertebrate DNA methylation and oxidation; however, much less is known about how modified cytosine residues within particular sequences are recognized. Among the known methylated DNA-binding domains, the Cys2-His2 zinc finger (ZnF) protein superfamily is the largest with hundreds of members, each containing tandem ZnFs ranging from 3 to >30 fingers. We have begun to biochemically and structurally characterize these ZnFs not only on their sequence specificity but also on their sensitivity to various DNA modifications. Rather than following published methods of refolding insoluble ZnF arrays, we have expressed and purified soluble forms of ZnFs, ranging in size from a tandem array of two to six ZnFs, from seven different proteins. We also describe a fluorescence polarization assay to measure ZnFs affinity with oligonucleotides containing various modifications and our approaches for cocrystallization of ZnFs with oligonucleotides., (© 2016 Elsevier Inc. All rights reserved.)

Single-molecule fluorescence imaging is a powerful tool that enables real-time observation of DNA-protein or RNA-protein interactions with a nanometer precision. Here, we provide a detailed procedure for a previously developed single-molecule fluorescence method, termed "single-molecule protein-induced fluorescence enhancement" (smPIFE). While smFRET (Förster resonance energy transfer) requires both donor and acceptor, protein-induced fluorescence enhancement (PIFE) employs a single dye and measures the increase in fluorescence intensity induced by protein binding near the dye. PIFE displays distance sensitivity within 0-4nm, making it a powerful complementary or alternative tool to FRET method. In this chapter, we will discuss the various ways that PIFE has been utilized to study protein-nucleic acid interactions., (© 2016 Elsevier Inc. All rights reserved.)

In this chapter, we describe a set of complementary techniques that we use to study the activation of rhodopsin, a G protein-coupled receptor (GPCR), and its functional interactions with G protein and arrestin. The protein reagents used for these studies come from native disc membranes or heterologous expression, and G protein and arrestin are often replaced with less complex synthetic peptides derived from key interaction sites of these binding partners (BPs). We first report on our approach to protein X-ray crystallography and describe how protein crystals from native membranes are obtained. The crystal structures provide invaluable resolution, but other techniques are required to assess the dynamic equilibria characteristic for active GPCRs. The simplest approach is "Extra Meta II," which uses UV/Vis absorption spectroscopy to monitor the equilibrium of photoactivated states. Site-specific information about the BPs (e.g., arrestin) is added by fluorescence techniques employing mutants labeled with reporter groups. All functional changes in both the receptor and interacting proteins or peptides are seen with highest precision using Fourier transform infrared (FTIR) difference spectroscopy. In our approach, the lack of site-specific information in FTIR is overcome by parallel molecular dynamics simulations, which are employed to interpret the results and to extend the timescale down to the range of conformational substates., (© 2015 Elsevier Inc. All rights reserved.)

The biology of an RNA is encoded in its structure and dynamics, whether that be binding to a protein, binding to another RNA, enzymatic catalysis, or becoming a substrate. In solution, most RNA molecules are sampling conformations, and their structures are best described as conformational ensembles. For larger RNAs, experiments that can describe the conformations of their domains can be particularly daunting, especially when the RNA is novel and not well characterized. Here, we explain how we have used site-specific 2-aminopurine as a fluorescent probe of the secondary and tertiary structures of a 60 nucleotide RNA, and what new findings we have about its Mg(2+)-dependent conformational changes. We focus on this RNA from prokaryotic ribosome as a proof of concept as well as a research project. Its tertiary structure is known from a cocrystal, and its secondary structure is modeled from phylogenetic conservation, but there are virtually no data describing the motions of its nucleotides in solution, or its folding kinetics. It is a perfect system to illustrate the unique information that comes from a comprehensive fluorescence study of this intricate RNA., (© 2015 Elsevier Inc. All rights reserved.)

In this chapter, we describe the currently most advanced methods applied for the quantitative assessment of ROS homeostasis inside the mitochondrion. These techniques are of particular interest in the field of oxidative stress. After discussing the importance of quantifying mitochondrial ROS homeostasis, three major aspects of this phenomenon and the pertinent methodologies for detection are delineated in detail. First the most important methods, based on fluorimetric or spectrophotometric approaches, for the detection of mitochondrial ROS are described. Elimination of ROS generated inside the mitochondrion is another crucial mechanism that also needs to be quantified accurately to estimate the antioxidant capacity of mitochondria under specific conditions. Since ROS generation and elimination manifest in concert, there needs to exist independent methods for the estimation of the net effect. Such a sensitive biochemical marker in the mitochondrion is aconitase, a citric acid cycle enzyme which is greatly sensitive to ROS. We describe two procedures for the precise determination of aconitase activity. A few auxiliary techniques and good practices having relevance in the successful accomplishment of the more delicate approaches are also mentioned. All other relevant technical considerations including advantages/disadvantages of the various methods and the most common artifacts are also discussed.

RNA and DNA carry out diverse functions in biology including catalysis, splicing, gene regulation, and storage of genetic information. Interest has grown in understanding how nucleic acids perform such sophisticated functions given their limited molecular repertoire. RNA can fold into diverse shapes that often perturb pKa values and allow it to ionize appreciably under biological conditions, thereby extending its molecular diversity. The goal of this chapter is to enable experimental measurement of pKa's in RNA and DNA. A number of experimental methods for measuring pKa values in RNA and DNA have been developed over the last 10 years, including RNA cleavage kinetics; UV-, fluorescence-, and NMR-detected pH titrations; and Raman crystallography. We begin with general considerations for choosing a pKa assay and then describe experimental conditions, advantages, and disadvantages for these assays. Potential pitfalls in measuring a pKa are provided including the presence of apparent pKa's due to a kinetic pKa or coupled acid- and alkali-promoted RNA unfolding, as well as degradation of RNA, precipitation of metal hydroxides and poor baselines. Use of multiple data fitting procedures and the study of appropriate mutants are described as ways to avoid some of these pitfalls. Application of these experimental methods to RNA and DNA will increase the number of available nucleic acid pKa values in the literature, which should deepen insight into biology and provide benchmarks for pKa calculations. Future directions for measuring pKa's in nucleic acids are discussed.

The Bcl-2 family proteins control apoptosis by regulation of outer mitochondrial membrane permeabilization. Studying the Bcl-2 family is particularly difficult because the functional interactions that regulate apoptosis occur at or within intracellular membranes. Compared to other biophysical methods, fluorescence spectroscopy is well suited to study membrane-bound proteins as experiments can be performed with intact membranes and at protein concentrations similar to those found in cells. For these reasons, fluorescence spectroscopy has been particularly useful in studying the regulation of membrane permeabilization by Bcl-2 family proteins. Here, we discuss four fluorescence-based assays used to study protein dynamics at membranes, with a focus on how these techniques can be used to study the Bcl-2 family proteins., (© 2014 Elsevier Inc. All rights reserved.)

Aerobic respiration is a major source of energy in eukaryotic cells. In this setting, ATP production by the mitochondrial respiratory chain relies on the availability of NADH and FADH2 to donate protons and electrons. The flux of electrons down the electron transport chain, based on a series of oxidation-reduction reactions, releases energy that allow for the transport of H(+) ions across the inner mitochondrial membrane. The resulting proton-motive force is employed to drive ATP synthesis, while the final acceptor of the electrons flowing through the respiratory chain if molecular oxygen. A side effect of this process is the generation of reactive oxygen species (ROS). While mitochondrial ROS (mtROS) production has been linked to many pathological conditions (i.e., aging and tumorigenesis), recent evidence suggests that multiple cells, including malignant cells, employ these by-products of energy production as signals to control various cellular processes. Here, we describe protocols to use chemical probes for measuring mtROS production in intact cells by flow cytometry and spectrofluorometry., (© 2014 Elsevier Inc. All rights reserved.)

Fluorescence correlation spectroscopy evaluates local signal fluctuations arising from stochastic movements of fluorescent particles in solution. The measured fluctuating signal is correlated in time and analyzed with appropriate model functions containing the parameters that describe the underlying molecular behavior. The dual-color extension, fluorescence cross-correlation spectroscopy (FCCS) allows for a comparison between spectrally well-separated channels to extract codiffusion events that reflect interactions between differently labeled molecules. In addition to solution measurements, FCCS can be applied with subcellular resolution and is therefore a very promising approach for a quantitative biochemical assessment of molecular networks in living cells. To derive thermodynamic and kinetic reaction parameters, the influence of a number of other factors like background noise, illumination intensity profiles, photophysical processes, and cross talk between the channels have to be treated. Here, we provide a roadmap to derive binding reaction data with dual-color FCCS using continuous wave laser excitation, as it is now accessible with many state-of-the-art confocal microscopes., (Copyright © 2013 Elsevier Inc. All rights reserved.)

Engineered nanoparticles (NPs) have found widespread application in technology and medicine. Whenever they come in contact with a living organism, interactions take place between the surfaces of the NPs and biomatter, in particular proteins, which are currently not well understood. We have introduced fluorescence correlation spectroscopy (FCS) and dual-focus FCS (2fFCS) to measure protein adsorption onto small NPs (~10-30 nm diameter). FCS allows us to measure, with subnanometer precision and as a function of protein concentration, the increase in hydrodynamic radius of the NPs due to protein adsorption. Investigations of the adsorption of a number of important serum proteins onto negatively charged, carboxyl-functionalized NPs revealed a stepwise increase of the NP size due to protein binding, clearly indicating that a protein monolayer enshrouds the NP. Structure-based calculations of the protein surface potentials reveal positively charged patches through which the proteins interact electrostatically with the negatively charged NP surfaces; the observed protein layer thickness is correlated with the molecular dimensions of the proteins binding in suitable orientations., (Copyright © 2013 Elsevier Inc. All rights reserved.)

Brightness analysis provides a powerful tool for the study of protein interactions both in solution and in living cells. We provide a brief survey of some widely used techniques for extracting brightness from fluorescent fluctuation spectroscopy experiments. While all the techniques are equivalent under ideal conditions, we touch upon their relative strengths and discuss in detail a specific scenario wherein the photon-counting histogram (PCH) separates the brightness of rare, bright particles from a dominant background. In a practical vein for ensuring quantitative and unbiased brightness data, we address a number of potential issues stemming from both theoretical assumptions and experimental realities. Two additional issues arising from geometry are examined in greater detail. An oil-immersion objective skews the geometry of the excitation volume as a function of penetration depth. The bias can be characterized and corrected or avoided through the use of a water-immersion objective. Brightness measurements in thin sample geometries, frequently encountered in cells, may be biased. We use z-scan FFS to characterize sample geometry and correct any resulting bias in the brightness., (Copyright © 2013 Elsevier Inc. All rights reserved.)

By FCS, a wide range of processes can be studied, covering time ranges from subnanoseconds to seconds. In principle, any process at equilibrium conditions can be measured, which reflects itself by a change in the detected fluorescence intensity. In this review, it is described how FCS and variants thereof can be used to monitor ion exchange, in solution and along biological membranes. Analyzing fluorescence fluctuations of ion-sensitive fluorophores by FCS offers selective advantages over other techniques for measuring local ion concentrations, and, in particular, for studying exchange kinetics of ions on a very local scale. This opens for several areas of application. The FCS approach was used to investigate fundamental aspects of proton exchange at and along biological membranes. The protonation relaxation rate, as measured by FCS for a pH-sensitive dye, can also provide information about local accessibility/interaction of a particular labeling site and conformational states of biomolecules, in a similar fashion as in a fluorescence quenching experiment. The same FCS concept can also be applied to ion exchange studies using other ion-sensitive fluorophores, and by use of dyes sensitive to other ambient conditions the concept can be extended also beyond ion exchange studies., (Copyright © 2013 Elsevier Inc. All rights reserved.)

Antibodies are excellent binding proteins that have found numerous applications in biological research, biotechnology, and medicine. Characterization of their ligand binding properties has long been, and continues to be, the focus of many researchers. Antibodies are also perfect test systems which can be used for the evaluation of newly introduced biophysical techniques. Working with many different antibodies, we continuously implement the growing arsenal of methods offered by fluorescence fluctuation spectroscopy (FFS) and apply them for antibody research. In this chapter, we will describe applications of FFS for antibody binding characterization and also provide examples how studying of antibodies helps to develop and enhance the tool set offered by FFS technology. In addition to traditional affinity evaluations, we will describe how resolving molecular populations enables determinations of the binding stoichiometry and provides further information about the system. Even though all our examples include antibodies, the same experimental procedures can also serve well for characterizing various proteins and other ligand binding systems., (Copyright © 2013 Elsevier Inc. All rights reserved.)

Fluorescence correlation spectroscopy (FCS) measures rates of transport (diffusion coefficients, convection velocities) and chemical reactions (rate constants) in equilibrium or nonequilibrium steady-state systems without the need for a perturbation of the state of the system. The rates are extracted from a record of fluorescence fluctuations observed from an open laser-illuminated observation volume. In addition, FCS provides the number of measured fluorescent molecules in the observation volume and, therefore, their molecular brightness. This enables sensitive measurements of aggregation of the fluorescent system components. FCS is now used as a routine tool for studying systems in physics, chemistry, and biology. Recent extensions of the fluorescence fluctuation approach have included methods based on imaging and cross correlation. Because of the sensitivity and chemical specificity of fluorescence detection and also the ability to form a very small diffraction-limited detection volume, FCS is especially useful for studies of dynamic molecular processes in living biological cells. FCS provides a window on mesoscopic systems and is closely related to fluorescence methods for studying single molecules., (Copyright © 2013 Elsevier Inc. All rights reserved.)

Cell-matrix adhesions are large, multimolecular complexes through which cells sense and respond to their environment. They also mediate migration by serving as traction points and signaling centers and allow the cell to modify the surroucnding tissue. Due to their fundamental role in cell behavior, adhesions are germane to nearly all major human health pathologies. However, adhesions are extremely complex and dynamic structures that include over 100 known interacting proteins and operate over multiple space (nm-μm) and time (ms-min) regimes. Fluorescence fluctuation techniques are well suited for studying adhesions. These methods are sensitive over a large spatiotemporal range and provide a wealth of information including molecular transport dynamics, interactions, and stoichiometry from a single time series. Earlier chapters in this volume have provided the theoretical background, instrumentation, and analysis algorithms for these techniques. In this chapter, we discuss their implementation in living cells to study adhesions in migrating cells. Although each technique and application has its own unique instrumentation and analysis requirements, we provide general guidelines for sample preparation, selection of imaging instrumentation, and optimization of data acquisition and analysis parameters. Finally, we review several recent studies that implement these techniques in the study of adhesions., (Copyright © 2013 Elsevier Inc. All rights reserved.)

Fluorescence correlation spectroscopy (FCS) is a technique in which measurement of fluorescence intensity fluctuations is used to clarify dynamic molecular interactions within a very small space in a solution containing a small number of fluorescent molecules. The FCS-based analysis gives the average number and average diffusion time of the fluorescent molecules during their passage through a very small space. One advantage of FCS is that physical separation between free and bound fluorescent probes is not required because the properties of fluorescence fluctuations are accounted for. Therefore, when fluorescent probes are bound with proteins by peroxidase and hydrogen peroxide (H2O2), FCS enables us to detect H2O2 with high sensitivity. In addition, because H2O2 is generated by oxidase-catalyzed reactions, a highly sensitive method for detecting H2O2 is applicable to the measurement of low levels of various oxidases and their substrates, such as glucose. We here describe the protocol of a de novo, highly sensitive method for the measurement of H2O2 and glucose using FCS., (Copyright © 2013 Elsevier Inc. All rights reserved.)

The Amplex Red assay, a fluorescent assay for the detection of H2O2, relies on the reaction of H2O2, which, in the presence of horseradish peroxidase, oxidizes the colorless, nonfluorescent, Amplex Red with a 1:1 stoichiometry to form the colored, fluorescent resorufin. We have found that resorufin is artifactually formed when Amplex Red is exposed to light. This photochemistry is initiated by trace amounts of resorufin present in Amplex Red stock solutions. ESR spin-trapping studies have demonstrated that superoxide radical is an intermediate in this process. Oxygen consumption measurements further confirmed that superoxide and H2O2 were artifactually produced by the photooxidation of Amplex Red. The artifactual formation of resorufin was also significantly increased by the presence of superoxide dismutase or HRP. This photooxidation process leads to a less sensitive assay for H2O2 under ambient light exposure and potentially invalid measurements under high energy exposure such as UVA irradiation. In general, precautions should be taken to minimize exposure to light, including that from instrumental light, during measurement of oxidative stress with Amplex Red., (Copyright © 2013 Elsevier Inc. All rights reserved.)

While intrinsic Brownian agitation within a lipid bilayer does homogenize the molecular distribution, the extremely diverse composition of the plasma membrane, in contrast, favors the development of inhomogeneity due to the propensity of such a system to minimize its total free energy. Precisely, deciphering such inhomogeneous organization with appropriate spatiotemporal resolution remains, however, a challenge. In accordance with its ability to accurately measure diffusion parameters, fluorescence correlation spectroscopy (FCS) has been developed in association with innovative experimental strategies to monitor modes of molecular lateral confinement within the plasma membrane of living cells. Here, we describe a method, namely spot variation FCS (svFCS), to decipher the dynamics of the plasma membrane organization. The method is based on questioning the relationship between the diffusion time τ(d) and the squared waist of observation w(2). Theoretical models have been developed to predict how geometrical constraints such as the presence of adjacent or isolated domains affect the svFCS observations. These investigations have allowed significant progress in the characterization of cell membrane lateral organization at the suboptical level, and have provided, for instance, compelling evidence for the in vivo existence of raft nanodomains., (Copyright © 2013 Elsevier Inc. All rights reserved.)

Time-integrated fluorescence cumulant analysis (TIFCA) is a data analysis technique for fluorescence fluctuation spectroscopy (FFS) that extracts information from the cumulants of the integrated fluorescence intensity. It is the first exact theory that describes the effect of sampling time on FFS experiment. Rebinning of data to longer sampling times helps to increase the signal/noise ratio of the experimental cumulants of the photon counts. The sampling time dependence of the cumulants encodes both brightness and diffusion information of the sample. TIFCA analysis extracts this information by fitting the cumulants to model functions. Generalization of TIFCA to multicolor FFS experiment is straightforward. Here, we present an overview of the theory, its implementation, as well as the benefits and requirements of TIFCA. The questions of why, when, and how to use TIFCA will be discussed. We give several examples of practical applications of TIFCA, particularly focused on measuring molecular interaction in living cells., (Copyright © 2013 Elsevier Inc. All rights reserved.)

Details of molecular membrane dynamics in living cells such as lipid-protein interactions or the incorporation of molecules into lipid "rafts" are often hidden to the observer because of the limited spatial resolution of conventional far-field optical microscopy. Fortunately, the superior spatial resolution of far-field stimulated-emission-depletion (STED) nanoscopy allows gaining new insights. Applying fluorescence correlation spectroscopy (FCS) in focal spots continuously tuned down to 30 nm in diameter distinguishes free from anomalous molecular diffusion due to transient binding, as for the diffusion of fluorescent phosphoglycero- and sphingolipid analogs in the plasma membrane of living cells. STED-FCS data recorded at different environmental conditions and on different lipid analogs reveal molecular details of the observed nanoscale trapping. Dependencies on the molecular structure of the lipids point to the distinct connectivity of the various lipids to initiate or assist cellular signaling events, but also outline strong differences to the characteristics of liquid-ordered and disordered phase separation in model membranes. STED-FCS is a highly sensitive and exceptional tool to study the membrane organization by introducing a new class of nanoscale biomolecular studies., (Copyright © 2013 Elsevier Inc. All rights reserved.)

This chapter introduces into the technique of dual-focus fluorescence correlation spectroscopy or 2fFCS. In 2fFCS, the fluorescence signals generated in two laterally shifted but overlapping focal regions are auto- and crosscorrelated. The resulting correlation curves are then used to determine diffusion coefficients of fluorescent molecules or particles in solutions or membranes. Moreover, the technique can also be used for noninvasively measuring flow-velocity profiles in three dimensions. Because the distance between the focal regions is precisely known and not changed by most optical aberrations, this provides an accurate and immutable external length scale for determining diffusivities and velocities, making 2fFCS the method of choice for accurately measuring absolute values of these quantities at pico- to nanomolar concentration., (Copyright © 2013 Elsevier Inc. All rights reserved.)

Fluorescence correlation spectroscopy (FCS) and related fluctuation spectroscopy and microscopy methods have become important research tools that enable detailed investigations of the chemical and physical properties of molecules and molecular systems in a variety of complex environments. Information recovery via curve fitting of fluctuation data can present complicating challenges due to limited resolution and/or problems with fitting model verification. We discuss a new approach to data analysis called τFCS that couples multiple modes of signal acquisition, here specifically FCS and fluorescence lifetimes, with global analysis. We demonstrate enhanced resolution using τFCS, including the capability to recover the concentration of both molecular species in a two-component mixture even when the species have identical diffusion coefficients and molecular brightness values, provided their fluorescent lifetimes are distinct. We also demonstrate how τFCS provides useful tools for model discrimination in FCS curve fitting., (Copyright © 2013 Elsevier Inc. All rights reserved.)

Fluorescence correlation spectroscopy (FCS) in combination with Förster resonance energy transfer (FRET) has been developed to a powerful statistical tool, which allows for the analysis of FRET fluctuations in the huge time of nanoseconds to seconds. FRET-FCS utilizes the strong distance dependence of the FRET efficiency on the donor (D)-acceptor (A) distance so that it developed to a perfect method for studying structural fluctuation in biomolecules involved in conformational flexibility, structural dynamics, complex formation, folding, and catalysis. Structural fluctuations thereby result in anticorrelated donor and acceptor signals, which are analyzed by FRET-FCS in order to characterize underlying structural dynamics. Simulated and experimental examples are discussed. First, we review experimental implementations of FRET-FCS and present theory for a two-state interconverting system. Additionally, we consider a very common case of FRET dynamics in the presence of donor-only labeled species. We demonstrate that the mean relaxation time for the structural dynamics can be easily obtained in most of cases, whereas extracting meaningful information from correlation amplitudes can be challenging. We present a strategy to avoid a fit with an underdetermined model function by restraining the D and A brightnesses of the at least one involved state, so that both FRET efficiencies and both rate constants (i.e., the equilibrium constant) can be determined. For samples containing several fluorescent species, the use of pulsed polarized excitation with multiparameter fluorescence detection allows for filtered FCS (fFCS), where species-specific correlation functions can be obtained, which can be directly interpreted. The species selection is achieved by filtering using fluorescence decays of individual species. Analytical functions for species auto- and cross-correlation functions are given. Moreover, fFCS is less affected by photophysical artifacts and often offers higher contrast, which effectively increases its time resolution and significantly enhances its capability to resolve multistate kinetics. fFCS can also differentiate between species even when their brightnesses are the same and thus opens up new possibilities to characterize complex dynamics. Alternative fluctuation algorithms to study FRET dynamics are also briefly reviewed., (Copyright © 2013 Elsevier Inc. All rights reserved.)

Fluorescence correlation spectroscopy (FCS) determines rates of molecular transport and chemical reactions from measurements of spontaneous concentration fluctuations in small open sub-volumes of systems in equilibrium or non-equilibrium steady state. The concentration fluctuations are monitored via fluorescence. Although difficult at first, FCS measurements are now in routine use in areas of chemistry, physics and biology. The initial approach has given rise to a wide range of extensions and variations that yield information about the dynamics of molecular processes in simple systems and living cells. FCS provides a window on a mesoscopic world in which molecular fluctuations are both detectable and (for biological cells) possibly functionally important. Moreover, FCS is a precursor to single molecule measurements., (Copyright © 2013 Elsevier Inc. All rights reserved.)

Fluorescence fluctuation techniques have proven to be extremely useful in the characterization of biomolecular interactions. Here an overview of recent applications of two-photon fluorescence fluctuation to the study of protein-nucleic acid complexes implicated in translational and transcriptional regulation is presented. In particular, the issue of the stoichiometry of the complexes is addressed using fluorescence (cross) correlation spectroscopy (F(C)CS) for the in vitro studies of one RNA-binding protein (the bacterial ribosomal protein L20) and two transcriptional repressors (CggR and CcpN, implicated in the control of the central carbon metabolism in Bacillus subtilis). Then, the application of two-photon scanning number and brightness (2psN&B) analysis of fluorescence microscopy measurements in single cells is presented. Multiple technical aspects related to the adaptation of this method to live bacteria are discussed. This approach was used to count the number of fluorescent protein molecules produced from different inducible promoters in B. subtilis reporter strains, in hundreds of individual cells under both permissive and repressive conditions. We present a case study in which the stochastic activity of glycolytic and gluconeogenic gene promoters could be quantified in vivo by 2psN&B and be related to the repression mechanisms proposed from in vitro studies., (Copyright © 2013 Elsevier Inc. All rights reserved.)

Communication between cells and their environment, including other cells, is often mediated by cell surface receptors. Fluorescence methodologies are among the most important techniques used to study receptors and their interactions, and in the past decade, fluorescence fluctuation spectroscopy (FFS) approaches have been increasingly utilized. In this overview, we illustrate how diverse FFS approaches have been used to elucidate important aspects of receptor systems, including interactions of receptors with their ligands and receptor oligomerization and clustering. We also describe the most popular methods used to introduce fluorescent moieties into the biological systems. Finally, specific attention will be given to cell maintenance and transfection strategies especially as related to microscopy studies., (Copyright © 2013 Elsevier Inc. All rights reserved.)