- Research article
- Open Access
Arbitrary protein−protein docking targets biologically relevant interfaces
© Martin and Lavery; licensee BioMed Central Ltd. 2012
Received: 6 January 2012
Accepted: 11 April 2012
Published: 6 May 2012
Protein-protein recognition is of fundamental importance in the vast majority of biological processes. However, it has already been demonstrated that it is very hard to distinguish true complexes from false complexes in so-called cross-docking experiments, where binary protein complexes are separated and the isolated proteins are all docked against each other and scored. Does this result, at least in part, reflect a physical reality? False complexes could reflect possible nonspecific or weak associations.
In this paper, we investigate the twilight zone of protein-protein interactions, building on an interesting outcome of cross-docking experiments: false complexes seem to favor residues from the true interaction site, suggesting that randomly chosen partners dock in a non-random fashion on protein surfaces. Here, we carry out arbitrary docking of a non-redundant data set of 198 proteins, with more than 300 randomly chosen "probe" proteins. We investigate the tendency of arbitrary partners to aggregate at localized regions of the protein surfaces, the shape and compositional bias of the generated interfaces, and the potential of this property to predict biologically relevant binding sites. We show that the non-random localization of arbitrary partners after protein-protein docking is a generic feature of protein structures. The interfaces generated in this way are not systematically planar or curved, but tend to be closer than average to the center of the proteins. These results can be used to predict biological interfaces with an AUC value up to 0.69 alone, and 0.72 when used in combination with evolutionary information. An appropriate choice of random partners and number of docking models make this method computationally practical. It is also noted that nonspecific interfaces can point to alternate interaction sites in the case of proteins with multiple interfaces. We illustrate the usefulness of arbitrary docking using PEBP (Phosphatidylethanolamine binding protein), a kinase inhibitor with multiple partners.
An approach using arbitrary docking, and based solely on physical properties, can successfully identify biologically pertinent protein interfaces.
It is now accepted as evident that protein-protein interactions (PPIs) are of fundamental importance in the vast majority of molecular events that occur in living organisms. Proteins can interact to form stable macromolecular assemblies that are able to perform many complex biological functions. They can also form transient interactions that collectively constitute dynamic networks of interactions that regulate how organisms operate. Protein-protein interactions are also of crucial importance to bacteria and viruses, which interfere with the host PPI network during infection [1, 2]. Logically, protein-protein binding sites are becoming major targets for novel drug design strategies .
Shape complementarity, surface hydrophobicity and charge complementarity have all been recognized as key factors of recognition in early studies [4, 5]. More recently, the increasing availability of structural data on protein-protein complexes  has led to a more refined picture of PPI mechanisms. Among the emerging structural and functional properties of transient interactions, one can cite conformational changes and disorder-to-order transitions upon interaction, the sequence conservation of interface residues, the existence of multi-specific proteins, and the role of post-translational modifications .
A number of methods for predicting PPIs have been developed, targeting two distinct aspects of the problem: protein-protein binding site prediction and protein docking. In the former case, the challenge is to identify the surface residues involved in the formation of protein-protein complexes; see [8–10] for recent reviews. In contrast, docking methods aim at predicting the structures of known, generally binary, complexes starting with the structures of separate proteins and using scoring functions based on shape/electrostatic/hydrophobic factors to locate optimal conformations. Substantial progress has been made in the docking field over recent years. The best algorithms are now able to predict correctly the structures of most complexes, when no major conformational change occurs during interaction, and promising developments are being made in the treatment of conformational changes [11, 12]. It has however been pointed out that the scoring functions used in docking perform very poorly when the aim is to predict binding affinities [13–15]. Notably, "cross-docking" studies, where binary protein complexes are separated and the isolated proteins are all docked against each other using a successful multiple minimization docking algorithm [15, 16], have demonstrated that it is very hard to distinguish between "true" (native) and "false" complexes. Similar difficulties were found using the top-performing Cluspro  web server [J. Martin unpublished results]. In another study, carried out on a larger scale, and using another docking algorithm , despite docking scores biased in favor of true complexes, the vast majority of cases led to false complexes being scored better than true ones.
The fact that false complexes obtain good scores during cross-docking studies raises two important and orthogonal questions: Are scoring functions so poor that they cannot discriminate interacting from non-interacting proteins (as suggested by the observations of [13, 14]), or does this result, at least in part, reflect a physical reality? Unfortunately, there is virtually no experimental data on the strength of the interactions comprising the "false" complexes. This set of complexes could potentially reflect potential weak, or nonspecific, interactions that are present in the cytoplasm, or avoided by mechanisms such as compartmentalization.
The fact that biological interactions in the cell are tightly orchestrated by localization and co-regulation mechanisms indeed suggests that significant nonspecific interactions may be common. It has been proposed that co-localization is necessary to control specific interactions, given the size of cells and the lifetime of individual proteins . So far, nonspecific interactions have only been marginally addressed in the literature, but they certainly deserve more attention. If localization and co-regulation is the rule in healthy cells, singular events also occur where localization breaks down, for example when mitochondrial proteins are released into the cytoplasm during the early phase of apoptosis, or when viral or bacterial proteins interfere with the host PPIs during infection. Recent studies indeed suggest that weak interactions play an important role in complex systems. A pioneering simulation of the bacterial cytoplasm has shown that proteins interacting with hard-sphere potentials diffuse too fast compared to experiment and that adding weak nonspecific attractions between all proteins could correct this behavior . Another recent study suggests that nonspecific binding acts as the evolutionary level to shape the PPI networks and limits the number of different proteins in genomes . Ultimately, a full understanding of proteins networks can only be achieved if we address the nonspecific as well as the specific interactions.
In this paper, we investigate what can be termed the "twilight zone" of protein-protein interactions, by using computational docking, and building on an interesting outcome of earlier cross-docking experiments: "false" complexes seem to favor interfaces containing residues belonging to "true" interaction sites [15, 18]. This suggests that randomly chosen protein partners dock in a non-random fashion. Using a non-redundant data set of 198 proteins, we explore the tendency of randomly chosen partners to aggregate at localized regions on the surface of each protein. We analyze the shape and compositional bias of the interfaces that are generated and the potential of this approach for predicting biologically relevant protein binding sites. We test our procedure on PEBP (Phosphatidylethanolamine binding protein), a kinase inhibitor with multiple known partners.
We have extracted protein structures from the docking benchmark data set assembled by Hwang et al., version 4.0 . This set consists of 176 binary protein complexes, for which structures of both partners in bound and unbound forms are available. These complexes are classified into functional categories (enzyme/inhibitor, antibody/antigen and "other") and according to the probable challenge for docking algorithms, which is related to conformational change upon complex formation (rigid body, medium difficulty and difficult). We first excluded the complexes from the antibody-antigen category (which do not display conventional PPI interfaces), and then reduced the redundancy level to 30% between protein chains using the PISCES web server . The final data set, denoted hereafter as the target data set, encompasses 198 proteins. Only unbound forms were used in all docking experiments. The structures were downloaded from http://zlab.umassmed.edu/benchmark/benchmark4.tgz.
These 198 proteins were docked against arbitrary partners taken from Nh3D, a data set of representative structures of each domain at the Topology level of the CATH structural classification database . Starting from version 3.0 of this data set (806 structures), we removed proteins with gaps in their backbone coordinates and proteins with high radius of gyration compared to their length (see Additional File 1).
To remove known structural interactions between arbitrary docking partners and the proteins from the target set, proteins classified in the same CATH Topology level as proteins of the benchmark 4.0 were removed. The final set includes 314 structures. It contains respectively 2, 91, 105, 53, 36 and 13 chains in length brackets ranging from 0–50 up to 250–300, and 14 chains with more than 300 residues. This data set is denoted as the compact probe data set. We further checked for known interactions between these probes and the target proteins using the IntAct database  and found only 16 interactions (see Additional File 1).
To investigate the role of structure compactness, we also considered a data set of 20 partners having a high radius of gyration compared to their length (see Additional File 1), denoted as the extended probe data set.
Docking was performed with the Hex software , version 6.3, which is adapted to GPU processors. Computations used the shape complementarity scoring function, with 18 and 25 expansion orders for the initial and final search steps (these orders control the precision of the molecular representation and influence the computation time). The full list of parameters is given in Additional File 1.Unless otherwise stated, we used only the best conformation of the complex produced by Hex.
Analysis of docking results
where min( N) and max( N) denote the minimum and maximum number of hits observed for each protein. Using this normalization, the number of hits per residue lies in the range [0,1].
The link between docking hits and surface shape was investigated using: (i) a local planarity analysis; (ii) the relative closeness to the geometrical center of the protein. The local planarity was measured with a planarity index, PIND, computed for each exposed residue as follows. Each residue was taken as the seed of a local surface patch, including all atoms of neighboring exposed residues within a 10 Å radius. To avoid discontinuities of these local surface patches (when for example, the radius selection includes residues from both sides of the protein), residues were filtered using hierarchical clustering with a single linkage procedure; the resulting tree was truncated using an empirical cutoff of 4.2 and secondary clusters were removed (see Additional File 1). PIND was then defined as the root mean squared distance of all atoms from the mean least squares plane . A low PIND denotes planar patches, while a high PIND denotes curved patches (pockets and protrusions). Each residue was also associated with a patch score, which is the mean number of normalized docking hits occurring in the patch around this residue.
To determine the closeness of an exposed residue to the geometric center (GEOCEN) of a protein, we built on the definition of Nicola and Vakser , by first reducing the protein to its Cα atoms. The relative closeness (RGEOCEN) of an exposed residue is then the ratio between its distance to the GEOCEN, and the mean distance of all exposed residues to the GEOCEN. A value below 1 consequently indicates that a residue is closer than average to the GEOCEN.
All statistical tests were performed using R . Docking hit distributions and random hit distributions were compared using the Cramer test, implemented in the Cramer package . We used this test rather than the Kolmogorov-Smirnov test because it can handle discrete distributions with ties .
The correlation between the number of docking hits and the patch planarity was measured using Pearson’s product moment correlation coefficient. Since the distributions we observe are not all Gaussian, we computed empirical p-values with 1000 replicates.
To take into account multiple testing, p-values were systematically corrected using the Benjamini-Hochberg method (BH) . Unlike the classical Bonferroni correction, the BH method controls the false discovery rate (proportion of significant cases that are false positives). With a risk level set to 5%, the probability to get at least one false discovery is 5% using the Bonferroni correction, whereas with the BH correction, the expected percentage of false discovery is 5%. Since we were more interested in the global number of significant p-values than the individual analysis of significant cases, we preferred the less stringent BH correction.
Where denotes the Chi-squared value obtained for the contingency table, and denotes the theoretical maximal Chi-squared of the contingency table, given by where N is the total count of the table and r and c are the table dimensions. Cramer’s V is, by construction, always between 0 (independence) and 1 (full dependence) and has a clear proportional interpretation: it is the fraction of the maximal departure from independence that one would observe in case of full dependence .
Biological interfaces were defined using the bound structures of the docking data set version 4.0  with a 5 Å distance cutoff between heavy atoms.
The performance in prediction was assessed using the False Positive Rate (FPR) and True Positive Rate (TPR) defined by and , where FP denotes the number of false positives (residues incorrectly predicted as interfacial), TN denotes the number of true negatives (residues outside the interface and rejected by the prediction), TP denotes the number of true positives (interface residues predicted as such) and FN denotes the number of false negatives (interface residues missed by the prediction). The computation of FPR and TPR for various thresholds enables a receiver operating characteristic (ROC) curve to be drawn. A unique measure of performance is then given by the resulting AUC value (area under the curve) that is equal to 0.5 for a random prediction and 1.0 for a perfect prediction. The prediction was carried out using exposed residues (RSA > 5%). AUC values were computed using the pROC package .
Comparison with other methods
VORFFIP is a recent and sophisticated method for predicting protein interaction surfaces which uses different forms of information including structural features, energy terms, evolutionary conservation and crystallographic B-factors, with a Voronoi-based environment description, combined in a two-step random forest classifier . The authors of this method kindly provided VORFFIP scores for the proteins in our target set.
JET is a method based on evolutionary trace . It uses a sampling of distance trees, and a post-processing clustering that takes into account physico-chemical properties as well as the evolutionary trace of the residues. We used the iterative version of JET with 10 iterations, and used the number of iterations where a given residue appeared in a cluster as a predictor (column ’clustersOccur’ of the _jet.res files).
Detection of multiple interfaces
PiQSi is a curated database of protein quaternary structures . Structures stored in PiQSi are manually examined and annotated as correct or incorrect, and it is possible to retrieve homologues of a given protein. Around 15% of the structures are annotated as erroneous. This resource was used to retrieve homologues of the target proteins involved in protein complexes and detect multiple interfaces. Structures were superimposed using PyMOL , which was also used to generate images of structures.
Docking hits target localized regions of protein surfaces
Extending the global analysis to individual proteins, we compute the distributions of observed and expected number of hits separately for each protein, and compare them with the Cramer test. The target proteins are binned in terms of their length range, and the number of significant p-values in each bin is shown in Figure 1C. For a total of 198 proteins, 150 have a significant p-value (<0.05), meaning that the distribution of docking hits on their surface significantly differs from random. There is a clear influence of protein size: shorter proteins tend to have non-significant p-values (implying random hits). A possible explanation is that smaller proteins get “saturated” faster than larger ones during docking with probes of various sizes. In other words, it is more difficult to target a precise site on the surface of a small protein using partners of diverse sizes. When docked with large partners, a significant portion of the surface will automatically be contacted; this suggests that small docking probes might be better adapted to detecting interaction interfaces on small proteins. To test this hypothesis, we divided the set of compact probes in half based on their size: we obtained 159 significant p-values out of 198 with the shortest probes, but only 133 significant p-values with the longest probes (versus 142 with half of the compact probes randomly chosen). This supports our hypothesis that small docking partners yield more significant p-values, and can detect localized interactions regions better, even on small protein targets.
The data shown on Figure 1 illustrate the first major result of this study: large-scale docking with a set of random partners, chosen to reflect the diversity of protein folds, reveals highly localized interaction regions on the surface of most of the target proteins. This is true both globally and individually for the set of 198 target proteins. These highly localized zones are termed “favored regions” and are the subject of further analysis below.
Docking hits do not accumulate on planar sites, or in pockets, but are generally close to the center of proteins
In this section, we explore the features of favored regions in terms of protein shape, using measures of local planarity and closeness to the geometrical center of the target proteins.
The local planarity around each exposed residue of the 198 target proteins is measured with the PIND planarity index described in the Methods section. The PIND of each residue is then compared with the corresponding patch score, which is the mean number of docking hits per residue in the local patch generated around the residue. To allow comparison among proteins of different size, the number of hits per exposed residue has to be normalized for each protein as explained in the Methods section. The global correlation between planarity index and patch score is very weak, with a Pearson correlation coefficient rho equal to −0.026 (empirical p-value < 0.001), implying that there is no link between local planarity and accumulated docking hits (see Additional File 1). This result is unchanged when the size of the local patches generated to measure the PIND is increased (rho = −0.057 with a distance cutoff equal to 15 Å).
Taken together, the result of local planarity analysis and the data presented in Figures 2 illustrate our second major finding: favored regions do not occur systematically on planar sites, or in pockets, or on protrusions, but do tend to prefer residues closer to the center of the protein than average (a feature previously demonstrated for the interfaces of known complexes ).
Docking hits prefer hydrophilic residues
This is the third result of our study: favored regions are weakly enriched in charged or hydrophilic residues.
Can arbitrary docking help to predict specific interfaces?
The logical extension of our finding is the use of the favored regions, generated by docking with random partners, to predict the location of native interfaces. The fact that false complexes can help to identify correct interfaces was noted in the first cross-docking experiment on twelve proteins , and visually assessed for ten proteins in the study of Wass et al. . Here, we quantify the predictive power of arbitrary docking on a larger data set, and assess its practical applications.
However, carrying out arbitrary docking against 314 random partners, even accelerated on GPUs, is a time-consuming procedure. To be usable in practice, it is desirable to find a way to reduce the computation time. In Figure 4B, we show that we can vary the number and size of the probe protein set, as well as the number of docking models, to decrease the amount of computation without damaging performance. We first tested reducing the number of probes used: the predictive power (assessed by the AUC) is not affected if we use only half of the compact probes randomly chosen, with an AUC equal to 0.666, but does decrease with further reductions. We also found that extended probes perform worse than compact ones (see Figure 4B): AUC is equal to 0.661 with 20 compact probes versus 0.650 with 20 extended probes. In terms of protein size, we found that when sorting the probes into two equal sets based on chain length, shorter chains function better (AUC is equal to 0.676 with short probes versus 0.651 with long probes) in agreement with the observation that smaller proteins can locate interfaces more precisely. Encouraged by this finding, we again decreased the size of the probe data set, but this time always keeping the shortest probes. In this case, the predictive power remained intact with as few as 75 probes, with an AUC equal to 0.678.
Lastly, we studied a third parameter: the number of docking models analyzed per probe. We found that the best performance (AUC = 0.682) is achieved using the first 10 models and only the 25 shortest probes. This suggests that arbitrary docking could be used in practical applications, since predictive power can be obtained with a very limited number of docking computations.
We now consider the performance of this approach compared with other existing methods (see Figure 4C). The first method we compared is VORFFIP . This method achieves an AUC equal to 0.795 on the target data set, whereas arbitrary docking, using 25 shortest probes and 10 models, achieved an AUC equal to 0.686. Since our method is based on only one feature, namely the information provided by arbitrary docking, we did not expect to equal the performance of a highly sophisticated multi-term method such as VORFFIP, which, today, can be considered to represent an upper bound on predictive power.
Next, we compared our performance to JET, which is based on sequence information, with a post-processing clustering . Using JET results, we achieved an AUC equal to 0.656. Since JET and arbitrary docking are based on two orthogonal sets of data (evolutionary versus physical), it seemed interesting to test a combination of the two predictors. A simple linear combination, with a weight equal to 0.6 for arbitrary docking and 0.4 for JET, led to an increase in AUC to 0.723. This very encouraging results shows that two features, conservation and arbitrary docking, can make very good predictions.
The fourth message of our study is therefore that arbitrary docking is computationally practical (with an appropriate choice of probes and docking models) and either alone, or combined with other data, provides significant information for predicting biologically-relevant protein interfaces.
Arbitrary docking can point to alternate interfaces
To extend this type of analysis to all the proteins of the target data set, we developed the procedure outlined in Figure 5B. We first used the PiQSi search engine to retrieve homologues of our proteins with more than 35% identity. We then restricted the set of homologues to the ones involved in protein complexes. At this stage, we excluded complexes annotated as errors or probable errors, but retained structures that are not yet annotated, which is the case for most of the proteins retrieved. This yielded a restricted set of 80 proteins that were subjected to further automatic and manual examination. We first automatically detected multiple interfaces: retrieved homologues were superimposed on the target proteins using the mapping information provided by PiQSi and interfaces were extracted using a 5 Å distance cutoff. A multiple interface was detected if more than 10 residues not belonging the native interface (the one present in the docking data set) were involved in another interface. In this way, we detected 59 proteins out of 80 as having multiple interfaces. These 59 proteins were visually inspected to see if arbitrary docking targeted the new interfaces. We found 31 such cases out of 59. The results are presented in Figure 5C, where proteins are ranked according to the quality of the predictions of the native interface. For the 45 proteins with a predictive signal lower than average, 20 cases with multiple interfaces are observed. This implies that the predictive power is actually underestimated for at least 20 of these proteins.
The data presented in Figure 5 illustrates the last message of our study: apparent failures of arbitrary docking in predicting biologically relevant interfaces may indicate alternative protein interaction sites.
A test case: PEBP
We conclude this study by showing the insight arbitrary docking can provide with a test case: the protein PEBP (Phosphatidylethanolamine binding protein). This protein, also called RKIP (Raf Kinase Inhibitor Protein), is a known inhibitor of several protein kinases, including those of the Raf/MEK/ERK pathways and the Aurora B pathway. PEBP also inhibits the GRK2 kinase, when activated by protein kinase C. These functionalities are the result of direct physical interactions, although no structural details of the complexes exist (personal communication from F. Schoentgen). Nevertheless, the structures of PEBP and some of its partners are available in the PDB. We thus subjected PEBP to arbitrary docking to highlight putative interaction sites, and also docked PEBP with its known partners using the Clus-Pro web server . We considered the following protein structures: human PEBP (PDB code 1BD9 , chain A), human B-Raf kinase (PDB code 3PRF ), human MEK1 (PDB code 3E8N ), human ERK1 (PDB code 2ZOQ , chain A), human TAK1 kinase-TAB1 fusion protein (PDB code 2EVA ), Xenopus aurora kinase (PDB code 2VGO , chain A), human protein kinase C-beta II (PDB code 2I0E , chain A) and human GRK2 (PDB code 3CIK, chain A). All these proteins are known to be functional as monomers (personal communication from F. Schoentgen), and we thus docked only monomeric forms, even if the biological unit from the PDB was not monomeric.
Lastly, it is interesting to contrast this study with other related research on protein binding sites. Here, we addressed a specific question: do computational docking experiments applied to random protein partners lead to specific bound conformations? We found that, generally, such conformations are not random and the interactions tend to favor specific sites on the protein surfaces. A similar behavior is observed for interactions between proteins and small molecules, both in vitro and in silico. In vitro, the multiple solvent crystal structures (MSCS) method involves solving the X-ray structure of a protein in different organic solvents. The solvent molecules effectively probe the protein surface and tend to form clusters at protein binding sites . In silico, the FTMAP algorithm has been developed to perform a fast Fourier surface mapping using the rigid-body docking of 16 small molecules with a given target protein .
Another notable feature of protein-protein interfaces is the uneven contribution of interface residues to the binding free energy. Generally, only a few residues, termed hot spots, make major contribution. Hot spot residues are enriched in tryptophan, tyrosine and arginine, but depleted in leucine, threonine and valine. They are preferentially located towards the center of the protein interface and appear in clusters [62–64]. There are, however, a number of protein-protein complexes that seem to be devoid of hot spots, and the hot spot nature of a residue may also change as a function of the surrounding protein interface . In the present study, we did not address the question of hot spots directly, but we did observe a consistent compositional bias favoring arginine and valine residues in regions targeted by docking hits. Further studies will be necessary to determine if hot spots make a significant contribution to the preferred protein complex conformations we have found.
We have shown that docking target proteins against an arbitrary set of proteins, leads to a non-random localization of interaction interfaces. These interfaces are neither systematically planar nor curved, but do tend to be closer than average to the center the protein. These predicted interfaces have been shown to contain information on the location of functional, biological interfaces, including alternative interfaces with multiple partners. An appropriate choice of random partners and of docking models analyzed makes arbitrary docking a practical tool for interface detection. The results can be used alone, or can complement data coming from other sources.
This study was not supported by any specific funding. We would like to thank David Ritchie for help with running Hex on GPUs and advise on choosing Hex parameters, Alexis Michon for technical help with cluster computations, Thomas Bourquard for useful discussion on the compositional bias of favored regions, Anne Lopes and Victoria Dimitrova for providing a recent version of the JET software and advice on choosing JET parameters and interpreting the results, Narcis Fernandez-Fuentes and Joan Segura Mora for providing the prediction data of the VORFIPP method, Françoise Schoentgen for providing the test case and structural information on PEBP and its interaction partners and finally Iris Martin Minard for her support during the manuscript revisions.
- Davey NE, Travé G, Gibson TJ: How viruses hijack cell regulation. Trends Biochem. Sci. 2011, 36: 159-169. 10.1016/j.tibs.2010.10.002.View ArticleGoogle Scholar
- de Curtis I: Host-Pathogen Interactions: Cheating the Host by Making New Connections. Current Biology. 2011, 21: R192-R194. 10.1016/j.cub.2011.01.041.View ArticleGoogle Scholar
- Wells JA, McClendon CL: Reaching for high-hanging fruit in drug discovery at protein-protein interfaces. Nature. 2007, 450: 1001-1009. 10.1038/nature06526.View ArticleADSGoogle Scholar
- Janin J, Miller S, Chothia C: Surface, subunit interfaces and interior of oligomeric proteins. Journal of Molecular Biology. 1988, 204: 155-164. 10.1016/0022-2836(88)90606-7.View ArticleGoogle Scholar
- Thornton JM, Singh J, Campbell S, Blundell TL: Protein-protein recognition via side-chain interactions. Biochem. Soc. Trans. 1988, 16: 927-930.View ArticleGoogle Scholar
- Berman HM, Westbrook J, Feng Z, Gilliland G, Bhat TN, Weissig H, Shindyalov IN, Bourne PE: The Protein Data Bank. Nucleic Acids Research. 2000, 28: 235-242. 10.1093/nar/28.1.235.View ArticleGoogle Scholar
- Perkins JR, Diboun I, Dessailly BH, Lees JG, Orengo C: Transient Protein-Protein Interactions: Structural, Functional, and Network Properties. Structure. 2010, 18: 1233-1243. 10.1016/j.str.2010.08.007.View ArticleGoogle Scholar
- Ezkurdia I, Bartoli L, Fariselli P, Casadio R, Valencia A, Tress ML: Progress and challenges in predicting protein-protein interaction sites. Brief. Bioinformatics. 2009, 10: 233-246.View ArticleGoogle Scholar
- de Vries SJ, Bonvin AMJJ: How proteins get in touch: interface prediction in the study of biomolecular complexes. Curr. Protein Pept. Sci. 2008, 9: 394-406. 10.2174/138920308785132712.View ArticleGoogle Scholar
- Zhou H-X, Qin S: Interaction-site prediction for protein complexes: a critical assessment. Bioinformatics. 2007, 23: 2203-2209. 10.1093/bioinformatics/btm323.View ArticleGoogle Scholar
- Zacharias M: Accounting for conformational changes during protein-protein docking. Curr. Opin. Struct. Biol. 2010, 20: 180-186. 10.1016/j.sbi.2010.02.001.View ArticleGoogle Scholar
- Lensink MF, Wodak SJ: Docking and scoring protein interactions: CAPRI 2009. Proteins. 2010, 78: 3073-3084. 10.1002/prot.22818.View ArticleGoogle Scholar
- Kastritis PL, Bonvin AMJJ: Are scoring functions in protein-protein docking ready to predict interactomes? Clues from a novel binding affinity benchmark. J. Proteome Res. 2010, 9: 2216-2225. 10.1021/pr9009854.View ArticleGoogle Scholar
- Kastritis PL, Moal IH, Hwang H, Weng Z, Bates PA: Bonvin AMJJ. 2011, A structure-based benchmark for protein-protein binding affinity. Protein Sci, Janin JGoogle Scholar
- Sacquin-Mora S, Carbone A, Lavery R: Identification of Protein Interaction Partners and Protein–Protein Interaction Sites. Journal of molecular biology. 2008, 382: 1276-1289. 10.1016/j.jmb.2008.08.002.View ArticleGoogle Scholar
- Zacharias M: Protein-protein docking with a reduced protein model accounting for side-chain flexibility. Protein Sci. 2003, 12: 1271-1282. 10.1110/ps.0239303.View ArticleGoogle Scholar
- Kozakov D, Hall DR, Beglov D, Brenke R, Comeau SR, Shen Y, Li K, Zheng J, Vakili P, Paschalidis IC, Vajda S: Achieving reliability and high accuracy in automated protein docking: Cluspro, PIPER, SDU, and stability analysis in CAPRI rounds 13–19. Proteins. 2010, 78: 3124-3130. 10.1002/prot.22835.View ArticleGoogle Scholar
- Wass MN, Fuentes G, Pons C, Pazos F, Valencia A: Towards the prediction of protein interaction partners using physical docking. Mol Syst Biol. 2011, 7: 469-View ArticleGoogle Scholar
- Batada NN, Shepp LA, Siegmund DO: Stochastic model of protein–protein interaction: Why signaling proteins need to be colocalized. Proceedings of the National Academy of Sciences of the United States of America. 2004, 101: 6445-6449. 10.1073/pnas.0401314101.View ArticleADSGoogle Scholar
- McGuffee SR, Elcock AH: Diffusion. Crowding & Protein Stability in a Dynamic Molecular Model of the Bacterial Cytoplasm. PLoS Comput Biol. 2010, 6: e1000694-Google Scholar
- Johnson ME, Hummer G: Nonspecific binding limits the number of proteins in a cell and shapes their interaction networks. Proceedings of the National Academy of Sciences. 2011, 108: 603-608. 10.1073/pnas.1010954108.View ArticleADSGoogle Scholar
- Hwang H, Vreven T, Janin J, Weng Z: Protein-protein docking benchmark version 4.0. Proteins. 2010, 78: 3111-3114. 10.1002/prot.22830.View ArticleGoogle Scholar
- Wang G, Dunbrack RL: PISCES: a protein sequence culling server. Bioinformatics. 2003, 19: 1589-1591. 10.1093/bioinformatics/btg224.View ArticleGoogle Scholar
- Thiruv B, Quon G, Saldanha S, Steipe B: Nh3D: A reference dataset of non-homologous protein structures. BMC Structural Biology. 2005, 5: 12-10.1186/1472-6807-5-12.View ArticleGoogle Scholar
- Kerrien S, Aranda B, Breuza L, Bridge A, Broackes-Carter F, Chen C, Duesbury M, Dumousseau M, Feuermann M, Hinz U, Jandrasits C, Jimenez RC, Khadake J, Mahadevan U, Masson P, Pedruzzi I, Pfeiffenberger E, Porras P, Raghunath A, Roechert B, Orchard S, Hermjakob H: The IntAct molecular interaction database in 2012. Nucleic Acids Research. 2011, 2011: 2011-Google Scholar
- Ritchie DW, Venkatraman V: Ultra-fast FFT protein docking on graphics processors. Bioinformatics. 2010, 26: 2398-2405. 10.1093/bioinformatics/btq444.View ArticleGoogle Scholar
- Hubbard SJ, Thornton JM: NACCESS. 2001, University College, London, 1Google Scholar
- Jones S, Thornton JM: Analysis of protein-protein interaction sites using surface patches. Journal of Molecular Biology. 1997, 272: 121-132. 10.1006/jmbi.1997.1234.View ArticleGoogle Scholar
- Nicola G, Vakser IA: A simple shape characteristic of protein–protein recognition. Bioinformatics. 2007, 23: 789-792. 10.1093/bioinformatics/btm018.View ArticleGoogle Scholar
- R Development Core Team: R: A Language and Environment for Statistical Computing. 2011, R Foundation for Statistical Computing, Vienna, AustriaGoogle Scholar
- Franz C: cramer. Multivariate nonparametric Cramer-Test for the two-sample-problem. 2006Google Scholar
- Baringhaus L, Franz C: On a new multivariate two-sample test. Journal of Multivariate Analysis. 2004, 88: 190-206. 10.1016/S0047-259X(03)00079-4.View ArticleMathSciNetGoogle Scholar
- Benjamini Y, Hochberg Y: Controlling the False Discovery Rate: A Practical and Powerful Approach to Multiple Testing. Journal of the Royal Statistical Society. Series B (Methodological). 1995, 57: 289-300.MathSciNetGoogle Scholar
- Acock AC, Gordon R: Stavig: A Measure of Association for Nonparametric Statistics. Social Forces. 1979, 57: 1381-1386.View ArticleGoogle Scholar
- DeLong ER, DeLong DM, Clarke-Pearson DL: Comparing the areas under two or more correlated receiver operating characteristic curves: a nonparametric approach. Biometrics. 1988, 44: 837-845. 10.2307/2531595.View ArticleGoogle Scholar
- Robin X, Turck N, Hainard A, Tiberti N, Lisacek F, Sanchez J-C, Müller M: pROC: an open-source package for R and S + to analyze and compare ROC curves. BMC Bioinformatics. 2011, 12: 77-10.1186/1471-2105-12-77.View ArticleGoogle Scholar
- Segura J, Jones P, Fernandez-Fuentes N: Improving the prediction of protein binding sites by combining heterogeneous data and Voronoi Diagrams. BMC Bioinformatics. 2011, 12: 352-10.1186/1471-2105-12-352.View ArticleGoogle Scholar
- Engelen S, Trojan LA, Sacquin-Mora S, Lavery R, Carbone A: Joint Evolutionary Trees: A Large-Scale Method To Predict Protein Interfaces Based on Sequence Sampling. PLoS Comput Biol. 2009, 5: e1000267-10.1371/journal.pcbi.1000267.View ArticleADSMathSciNetGoogle Scholar
- Levy ED: PiQSi: Protein Quaternary Structure Investigation. Structure. 2007, 15: 1364-1367. 10.1016/j.str.2007.09.019.View ArticleGoogle Scholar
- The PyMOL molecular graphics system: San Carlos. 2002, DeLano Scientific, CA, USAGoogle Scholar
- Lang HLE, Jacobsen H, Ikemizu S, Andersson C, Harlos K, Madsen L, Hjorth P, Sondergaard L, Svejgaard A, Wucherpfennig K, Stuart DI, Bell JI, Jones EY, Fugger L: A functional and structural basis for TCR cross-reactivity in multiple sclerosis. Nat Immunol. 2002, 3: 940-943. 10.1038/ni835.View ArticleGoogle Scholar
- Sundberg EJ, Sawicki MW, Southwood S, Andersen PS, Sette A, Mariuzza RA: Minor structural changes in a mutated human melanoma antigen correspond to dramatically enhanced stimulation of a CD4+ tumor-infiltrating lymphocyte line. J. Mol. Biol. 2002, 319: 449-461. 10.1016/S0022-2836(02)00370-4.View ArticleGoogle Scholar
- Simader H, Hothorn M, Suck D: Structures of the interacting domains from yeast glutamyl-tRNA synthetase and tRNA-aminoacylation and nuclear-export cofactor Arc1p reveal a novel function for an old fold. Acta Crystallographica Section D Biological Crystallography. 2006, 62: 1510-1519. 10.1107/S0907444906039850.View ArticleGoogle Scholar
- Simader H, Hothorn M, Köhler C, Basquin J, Simos G, Suck D: Structural basis of yeast aminoacyl-tRNA synthetase complex formation revealed by crystal structures of two binary sub-complexes. Nucleic Acids Research. 2006, 34: 3968-3979. 10.1093/nar/gkl560.View ArticleGoogle Scholar
- Bella J, Kolatkar PR, Marlor CW, Greve JM, Rossmann MG: The structure of the two amino-terminal domains of human ICAM-1 suggests how it functions as a rhinovirus receptor and as an LFA-1 integrin ligand. Proc. Natl. Acad. Sci. U.S.A. 1998, 95: 4140-4145. 10.1073/pnas.95.8.4140.View ArticleADSGoogle Scholar
- Shimaoka M, Xiao T, Liu J-H, Yang Y, Dong Y, Jun C-D, McCormack A, Zhang R, Joachimiak A, Takagi J, Wang J-H, Springer TA: Structures of the alpha L I domain and its complex with ICAM-1 reveal a shape-shifting pathway for integrin regulation. Cell. 2003, 112: 99-111. 10.1016/S0092-8674(02)01257-6.View ArticleGoogle Scholar
- Stroupe C, Brunger AT: Crystal structures of a Rab protein in its inactive and active conformations. J. Mol. Biol. 2000, 304: 585-598. 10.1006/jmbi.2000.4236.View ArticleGoogle Scholar
- Ignatev A, Kravchenko S, Rak A, Goody RS, Pylypenko O: A Structural Model of the GDP Dissociation Inhibitor Rab Membrane Extraction Mechanism. Journal of Biological Chemistry. 2008, 283: 18377-18384. 10.1074/jbc.M709718200.View ArticleGoogle Scholar
- Ko TP, Liao CC, Ku WY, Chak KF, Yuan HS: The crystal structure of the DNase domain of colicin E7 in complex with its inhibitor Im7 protein. Structure. 1999, 7: 91-102. 10.1016/S0969-2126(99)80012-4.View ArticleGoogle Scholar
- Huang H, Yuan HS: The conserved asparagine in the HNH motif serves an important structural role in metal finger endonucleases. J. Mol. Biol. 2007, 368: 812-821. 10.1016/j.jmb.2007.02.044.View ArticleGoogle Scholar
- Hsieh SY, Ko TP, Tseng MY, Ku W, Chak KF, Yuan HS: A novel role of ImmE7 in the autoregulatory expression of the ColE7 operon and identification of possible RNase active sites in the crystal structure of dimeric ImmE7. EMBO J. 1997, 16: 1444-1454. 10.1093/emboj/16.6.1444.View ArticleGoogle Scholar
- Banfield MJ, Barker JJ, Perry AC, Brady RL: Function from structure? The crystal structure of human phosphatidylethanolamine-binding protein suggests a role in membrane signal transduction. Structure. 1998, 6: 1245-1254. 10.1016/S0969-2126(98)00125-7.View ArticleGoogle Scholar
- Ren L, Wenglowsky S, Miknis G, Rast B, Buckmelter AJ, Ely RJ, Schlachter S, Laird ER, Randolph N, Callejo M, Martinson M, Galbraith S, Brandhuber BJ, Vigers G, Morales T, Voegtli WC, Lyssikatos J: Non-oxime inhibitors of B-Raf(V600E) kinase. Bioorg. Med. Chem. Lett. 2011, 21: 1243-1247. 10.1016/j.bmcl.2010.12.061.View ArticleGoogle Scholar
- Iverson C, Larson G, Lai C, Yeh L-T, Dadson C, Weingarten P, Appleby T, Vo T, Maderna A, Vernier J-M, Hamatake R, Miner JN, Quart B: RDEA119/BAY 869766: a potent, selective, allosteric inhibitor of MEK1/2 for the treatment of cancer. Cancer Res. 2009, 69: 6839-6847. 10.1158/0008-5472.CAN-09-0679.View ArticleGoogle Scholar
- Kinoshita T, Yoshida I, Nakae S, Okita K, Gouda M, Matsubara M, Yokota K, Ishiguro H, Tada T: Crystal structure of human mono-phosphorylated ERK1 at Tyr204. Biochem. Biophys. Res. Commun. 2008, 377: 1123-1127. 10.1016/j.bbrc.2008.10.127.View ArticleGoogle Scholar
- Brown K, Vial SCM, Dedi N, Long JM, Dunster NJ, Cheetham GMT: Structural Basis for the Interaction of TAK1 Kinase with its Activating Protein TAB1. Journal of Molecular Biology. 2005, 354: 1013-1020. 10.1016/j.jmb.2005.09.098.View ArticleGoogle Scholar
- D’Alise AM, Amabile G, Iovino M, Di Giorgio FP, Bartiromo M, Sessa F, Villa F, Musacchio A, Cortese R: Reversine, a novel Aurora kinases inhibitor, inhibits colony formation of human acute myeloid leukemia cells. Molecular Cancer Therapeutics. 2008, 7: 1140-1149. 10.1158/1535-7163.MCT-07-2051.View ArticleGoogle Scholar
- Grodsky N, Li Y, Bouzida D, Love R, Jensen J, Nodes B, Nonomiya J, Grant S: Structure of the catalytic domain of human protein kinase C beta II complexed with a bisindolylmaleimide inhibitor. Biochemistry. 2006, 45: 13970-13981. 10.1021/bi061128h.View ArticleGoogle Scholar
- Serre L, Vallée B, Bureaud N, Schoentgen F, Zelwer C: Crystal structure of the phosphatidylethanolamine-binding protein from bovine brain: a novel structural class of phospholipid-binding proteins. Structure. 1998, 6: 1255-1265. 10.1016/S0969-2126(98)00126-9.View ArticleGoogle Scholar
- Mattos C, Ringe D: Locating and characterizing binding sites on proteins. Nature Biotechnology. 1996, 14: 595-599. 10.1038/nbt0596-595.View ArticleGoogle Scholar
- Brenke R, Kozakov D, Chuang G-Y, Beglov D, Hall D, Landon MR, Mattos C, Vajda S: Fragment-Based Identification of Druggable ‘hot Spots’ of Proteins Using Fourier Domain Correlation Techniques. Bioinformatics. 2009, 25: 621-627. 10.1093/bioinformatics/btp036.View ArticleGoogle Scholar
- Moreira IS, Fernandes PA, Ramos MJ: Hot spots-A review of the protein-protein interface determinant amino-acid residues. Proteins. 2007, 68: 803-812. 10.1002/prot.21396.View ArticleGoogle Scholar
- Bogan AA, Thorn KS: Anatomy of hot spots in protein interfaces. Journal of Molecular Biology. 1998, 280: 1-9. 10.1006/jmbi.1998.1843.View ArticleGoogle Scholar
- Bonsor DA, Sundberg EJ: Dissecting Protein − Protein Interactions Using Directed Evolution. Biochemistry. 2011, 50: 2394-2402. 10.1021/bi102019c.View ArticleGoogle Scholar
This article is published under license to BioMed Central Ltd. This is an Open Access article distributed under the terms of the Creative Commons Attribution License (http://creativecommons.org/licenses/by/2.0), which permits unrestricted use, distribution, and reproduction in any medium, provided the original work is properly cited.