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New Methods for the Study of Protein–Nucleic Acid Interactions Time-resolved footprinting for the study of the structural dynamics of DNA–protein interactions Bianca Sclavi1 LBPA (Laboratoire de Biotechnologies et Pharmacologie génétique Appliquée), UMR 8113 du CNRS, Ecole Normale Supérieure de Cachan, Cachan, France Abstract Transcription is often regulated at the level of initiation by the presence of transcription factors or nucleoid proteins or by changing concentrations of metabolites. These can influence the kinetic properties and/or structures of the intermediate RNA polymerase–DNA complexes in the pathway. Time-resolved footprinting techniques combine the high temporal resolution of a stopped-flow apparatus with the specific structural information obtained by the probing agent. Combined with a careful quantitative analysis of the evolution of the signals, this approach allows for the identification and kinetic and structural characterization of the intermediates in the pathway of DNA sequence recognition by a protein, such as a transcription factor or RNA polymerase. The combination of different probing agents is especially powerful in revealing different aspects of the conformational changes taking place at the protein–DNA interface. For example, hydroxyl radical footprinting, owing to their small size, provides a map of the solvent-accessible surface of the DNA backbone at a single nucleotide resolution; modification of the bases using potassium permanganate can reveal the accessibility of the bases when the double helix is distorted or melted; cross-linking experiments report on the formation of specific amino acid–DNA contacts, and DNase I footprinting results in a strong signal-to-noise ratio from DNA protection at the binding site and hypersensitivity at curved or kinked DNA sites. Recent developments in protein footprinting allow for the direct characterization of conformational changes of the proteins in the complex. Several methods exist for the quantitative study of the complexes formed between proteins and their specific sites on DNA. Each method brings a different level of detail and unique information on the structural signatures of the complex. For a complete characterization of a complex, the use of a few different complementary techniques is often necessary. In this paper, I will describe the use of footprinting methods for the equilibrium and kinetic characterization of DNA– protein complexes. Footprinting is a general term that refers to those techniques that rely on the comparative modification of the polynucleotide in the presence or absence of a binding molecule, a drug or a protein. Footprinting techniques are also applied to the study of RNA structure and RNA folding [1,2] and, more recently, have been applied to the measurement of solvent-accessible surfaces of proteins [3]. Briefly, a fragment of DNA, for example, is cleaved or modified by a chemical agent or enzyme at all accessible sites. When the same reaction is carried out in the presence of the binding partner, such as a protein, the sites involved in the interactions will, in general, become protected from cleavage or modification. The resulting DNA fragments are separated and identified by denaturing gel electrophoresis and the extent of the resulting cleavage pattern can be quantified. The same kind of experiment can be carried out on a supercoiled plasmid. In this case, primer extension is used to Key words: DNA–protein interaction, equilibrium experiment, footprinting, kinetic experiment, structural dynamics, time-resolved experiment. 1 email [email protected] Biochem. Soc. Trans. (2008) 36, 745–748; doi:10.1042/BST0360745 identify the sites of cleavage or modification [4]. The primer extension by a thermostable DNA polymerase can be done in a PCR machine, thus obtaining a linear amplification of the signal. This is particularly useful for detection of in vivo footprints both on plasmids and on chromosomal DNA [5,6]. In order to carry out a quantitative analysis, it is necessary to have identified at least a region of binding of the protein on the DNA. This is often obtained by a gel shift assay using different fragments of the putative binding region. Once a specifically bound fragment is identified, footprinting techniques can be used to identify the location of the binding site(s). In the case in which the consensus binding sequence is known, the fragment containing this sequence is selected. In addition, it is necessary to obtain a sample of the purified protein of interest. Equilibrium experiments Equilibrium experiments are used to measure the affinities and co-operativity of binding. In this case, the DNA is kept at a fixed concentration, while the concentration of the protein is gradually increased. In order to measure a binding affinity, the concentration of the DNA should be lower than the K d (affinity equilibrium constant) and the protein concentration should be in large excess so that the amount of free protein does not change significantly during the titration; this simplifies the subsequent analysis. If the concentration of DNA is above the K d , one can measure the stoichiometry of binding. C The C 2008 Biochemical Society Authors Journal compilation 745 746 Biochemical Society Transactions (2008) Volume 36, part 4 Kinetic experiments Kinetic experiments are used to measure the rates of complex formation and to identify the presence and the structure of possible intermediates in the binding pathway. For these experiments, the protein and DNA are mixed and the complex is probed after increasing incubation times until equilibrium is reached. In this case, an excess of protein over DNA equally ensures small changes in the amount of free protein and concentrations of protein at least ten times greater than the K d ensure that the binding site is saturated and the signal is at its highest level. For this reason kinetic experiments usually follow an equilibrium characterization. In order to carry out time-resolved footprinting experiments, the use of a stopped-flow apparatus with a dead time of 20–50 ms may be necessary if the reaction is completed within several seconds [7]. The manual mixing and reaction time is usually limited to 10–30 s and can be used to measure timescales in the order of several minutes. Three main methods have been described to produce hydroxyl radicals [10]. The first is the Fenton reaction, which requires chelated iron, H2 O2 and often a reducing agent such as ascorbate to reduce the iron. The second is peroxynitrous acid, which, however, is very sensitive to the pH of the buffer [14]. The third is from the radiolysis of water-induced γ - or X-ray radiation. All of these methods have been used for both equilibrium and time-resolved experiments [15]. A variant of the Fenton reaction is the binding of the iron by a BABE (bromoacetamidobenzyl-EDTA) molecule that has been added to a specific site on the protein of interest. This approach has been used for both protein–DNA and protein–protein interactions and it is especially useful to place a specific protein domain with respect to the DNA-binding sequence or another protein partner [16,17]. Exposure of live or frozen cells to γ - or X-ray radiation can be used to obtain in vivo footprints of protein–DNA complexes or RNA structures [6,18]. UV laser cross-linking Footprinting techniques DNase I DNase I is an enzyme that cleaves the DNA from the minor groove with a slight sequence and structural preference. For example, AT-rich regions are cut with decreased efficiency, whereas sequences that are curved or kinked towards the major groove are cut with a higher efficiency due to increased affinity of the enzyme for these structures [8]. This results in the appearance of hypersensitive cleavage sites. DNase I experiments result in a high signal-to-noise ratio and report on the presence of curved or kinked structures; however, the size of the binding site for the enzyme and the steric clash between DNase I and the protein bound to the DNA results in a low spatial resolution. Equilibrium footprinting and time-resolved quantitative DNase I footprinting have been used for the study of the affinity, co-operativity and kinetics of binding of proteins, most often transcription factors, to DNA [9]. Hydroxyl radical footprinting Hydroxyl radicals are small and highly reactive. They abstract a proton from the sugar in the polynucleotide backbone, resulting in a radical rearrangement and a break in the DNA or RNA strand in virtually a sequence-independent reaction [10]. Because of their small size, about the same as a water molecule, the resulting cleavage pattern shows a good correlation with the solvent accessibility of the backbone [11]. This is influenced by the sequence-dependent helical structure, particularly at long stretches of adenines or thymines resulting in a reduced minor groove width. The main advantage of hydroxyl radical footprints is thus a high structural resolution of the protection pattern. This pattern has often been used to build molecular models of the structure of the DNA–protein complex or of tertiary RNA structure [12,13]. C The C 2008 Biochemical Society Authors Journal compilation UV laser cross-linking is based on the modification of DNA bases after their absorption of UV light [19]. This can occur by the formation of thymine dimers or guanosine oxidation. If the DNA structure were modified by the binding of a protein, the probability of the formation of these modifications may be altered; in addition, if an amino acid were in close contact with a base, a covalent bond may result from the UV absorption. These modifications are detected by a primer extension reaction that can be carried out using a thermostable polymerase in a PCR machine for a linear amplification of the signal. In addition, the formation of a covalent bond between the protein and the DNA allows for the identification of the peptide or even the amino acid on the protein involved in that interaction [19]. This may require the use of MS analysis of the protein sample after digestion of the DNA fragment. By using a UV laser instead of a common UV lamp, the exposure time of the sample is significantly reduced from a few minutes to a few nanoseconds. A further advantage of UV cross-linking is that it can be carried out on live cells. The DNA is subsequently extracted and the primer extension can be used to detect whether a protein was bound to the DNA at the time of exposure in vivo (see for example [5,20]). The yield of cross-links on unmodified DNA is usually very low, approx. 0.5%; however, it can be increased by a modification of the DNA bases or backbone (see for example [21]). DMS and potassium permanganate footprinting Both DMS and potassium permanganate can be used to measure the conformational changes of individual bases from the canonical B helix structure of DNA. They are part of a large family of chemical reagents that can be used to probe different structural aspects of the bases within polynucleotide chains. DMS reacts preferably with G>C, depending on the reaction conditions, resulting in a methylation of the base that can be detected either by primer extension or by reaction New Methods for the Study of Protein–Nucleic Acid Interactions with a strong base. Potassium permanganate instead reacts preferably with T>C. Both of these techniques have been used to measure the degree of melting of the double helix by temperature or the presence of specific proteins such as RNA polymerase (see for example [22–24]). When used quantitatively, one must be careful to distinguish changes in the accessibility of the base from changes to its intrinsic reactivity [25]. In addition, full double-strand melting may not be necessary to observe an increase in reactivity; a distortion of the DNA may be sufficient to obtain a signal. fragment, in the order of a few nanomolar. The use of capillary sequencers to obtain footprinting data and semi-automated peak-fitting software had resulted in a considerable decrease in the time necessary to analyse the samples and have increased confidence and reproducibility of the results [2]. Finally, a careful quantitative characterization of the affinities and rates in the formation of DNA–protein complexes is necessary if one wants to create a model of the regulatory network in order to describe its dynamics and/or the mechanisms of regulation [28]. Quantitative analysis In order to carry out a quantitative analysis of the extent of modification or cleavage for a footprinting experiments, a few conditions should be met. First of all, no more than 30% of the molecule should be cleaved or modified in order to ensure that the reaction is within single hit regime, meaning that each molecule is not cleaved or modified more than once. In addition, as described above, it is better to work with a concentration of DNA below the K d and an excess of protein concentration. The main reason for the latter is that the equations that are used to fit the binding curves are based on the assumption that the amount of free protein in solution does not change from one sample to the next (for a review, see [2]). An internal standard of an unmodified region is often used in order to decrease the noise in the data due to losses of material during sample purification and gel loading. This may become more difficult in the case of potassium permanganate footprinting, where it is rare that bases become modified in the absence of protein or in the case where the whole length of the DNA becomes protected by the protein. In these cases, one can sometimes control the amount of material that is loaded on to the gel or normalize for the total amount of DNA in the sample. In some cases, one can add a standard fragment of DNA that migrates in the gel far from the bands of interest and is not affected by the presence of the protein. Once a measure of the change in reactivity of the different sites is obtained, it can be fit to a binding equation, in the case of equilibrium experiments, or for time-resolved experiments to a single, double and sometimes even triple exponential equations. As the number of exponents, and therefore of parameters, increases, one should use statistical tests in order to determine whether the increase in the goodness to fit is significant. The changes in the amplitudes corresponding to the different phases can be used to measure the relative amount of each intermediate [26,27]. The quantification of the band intensities on a polyacrylamide gel can be obtained by exposing the gel to a phosphoimager screen in order to digitize the image and by using the quantification software available with the imaging apparatus [2]. More recently, the use of fluorescently labelled DNA has become more popular as the detection sensitivity of capillary sequencers has improved. 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