- Research article
- Open Access
Role of the highly conserved G68 residue in the yeast phosphorelay protein Ypd1: implications for interactions between histidine phosphotransfer (HPt) and response regulator proteins
BMC Biochemistry volume 20, Article number: 1 (2019)
Many bacteria and certain eukaryotes utilize multi-step His-to-Asp phosphorelays for adaptive responses to their extracellular environments. Histidine phosphotransfer (HPt) proteins function as key components of these pathways. HPt proteins are genetically diverse, but share a common tertiary fold with conserved residues near the active site. A surface-exposed glycine at the H + 4 position relative to the phosphorylatable histidine is found in a significant number of annotated HPt protein sequences. Previous reports demonstrated that substitutions at this position result in diminished phosphotransfer activity between HPt proteins and their cognate signaling partners.
We report the analysis of partner binding interactions and phosphotransfer activity of the prototypical HPt protein Ypd1 from Saccharomyces cerevisiae using a set of H + 4 (G68) substituted proteins. Substitutions at this position with large, hydrophobic, or charged amino acids nearly abolished phospho-acceptance from the receiver domain of its upstream signaling partner, Sln1 (Sln1-R1). An in vitro binding assay indicated that G68 substitutions caused only modest decreases in affinity between Ypd1 and Sln1-R1, and these differences did not appear to be large enough to account for the observed decrease in phosphotransfer activity. The crystal structure of one of these H + 4 mutants, Ypd1-G68Q, which exhibited a diminished ability to participate in phosphotransfer, shows a similar overall structure to that of wild-type. Molecular modelling suggests that the highly conserved active site residues within the receiver domain of Sln1 must undergo rearrangement to accommodate larger H + 4 substitutions in Ypd1.
Phosphotransfer reactions require precise arrangement of active site elements to align the donor-acceptor atoms and stabilize the transition state during the reaction. Any changes likely result in an inability to form a viable transition state during phosphotransfer. Our data suggest that the high degree of evolutionary conservation of residues with small side chains at the H + 4 position in HPt proteins is required for optimal activity and that the presence of larger residues at the H + 4 position would cause alterations in the positioning of active site residues in the partner response regulator.
Histidine phosphotransfer (HPt) proteins allow bacteria, yeast, and plants to expand beyond canonical two-component signaling pathways into multi-step phosphorelay pathways. These signaling proteins play crucial roles in regulating numerous cellular functions including those essential for growth and viability [1,2,3,4]. In bacteria, HPt domains are often additional domains embedded in histidine kinases of two-component signaling pathways [5,6,7]. In fungi and plants, HPts are typically stand-alone proteins that occupy branch points within multi-step His-to-Asp phosphorelays [8,9,10,11].
Multi-step phosphorelay systems consist of an upstream hybrid sensor histidine kinase (HHK), an HPt protein, and often multiple downstream response regulators (RR). Signal transduction is initiated when an external stimulus sensed by the HHK results in conformational changes that shift the protein from an inactive to an active conformation [12,13,14]. Phosphoryl transfer proceeds in a His-Asp-His-Asp manner, capitalizing on the chemical labilities of phospho-histidine and phospho-aspartate. Transfer of the γ-phosphate of adenosine triphosphate (ATP) occurs by autophosphorylation on a conserved histidine residue on the HHK, followed by transfer of the same phosphoryl group to a conserved aspartate residue on the receiver domain of the HHK. The HPt protein (or domain) acts as an intermediate in the signaling pathway by transferring the phosphoryl group from the HHK to a RR, which elicits a cellular response to the detected stress [1, 15, 16].
The Sln1 multi-step His-to-Asp phosphorelay of Saccharomyces cerevisiae has been extensively studied [17,18,19,20]. The pathway consists of the transmembrane HHK Sln1, the HPt Ypd1, and the RR proteins Ssk1 and Skn7 [11, 20,21,22]. According to the Saccharomyces Genome Database, Ypd1 is encoded by a single copy gene on chromosome IV, Ssk1 on chromosome XII, and Skn7 on chromosome VIII . While Ypd1 has only a single upstream activator, it can phosphorylate both downstream RR proteins (Ssk1 and Skn7), depending on the encountered stress. Ssk1 is responsible for the osmotic stress response through the High Osmolarity Glycerol (HOG1) Mitogen Activated Protein Kinase (MAPK) pathway, while Skn7 is responsible for cell wall stress response and functions through direct transcriptional regulation of cell wall-related genes [24, 25]. Ypd1 is located in the cytoplasm of the cell, along with Ssk1, while Skn7 is sequestered in the nucleus . Ypd1 readily translocates into the nucleus upon cell wall stress to phosphorylate Skn7 . Under normal osmotic conditions, the Sln1-Ypd1-Ssk1 branch of the pathway is constitutively phosphorylated, and the downstream HOG1 pathway is repressed. Under hyperosmotic stress, Sln1 ceases to autophosphorylate, allowing dephosphorylated Ypd1 and Ssk1 to accumulate and activate the HOG1 pathway [27, 28]. The net result of HOG1 pathway activation is the production of intracellular glycerol that acts as a counter osmolyte [29, 30]. The Sln1 pathway is required for cell viability through regulation of the HOG1 pathway [11, 21, 31]. Defects in any step of the Sln1 pathway compromise the cell’s ability to respond to osmotic stress, leading to decreased cell viability [11, 27, 32].
Previous studies of the Sln1 pathway using yeast two-hybrid assays and X-ray crystallography demonstrated that Ypd1 interacts with the receiver domains of its response regulator binding partners using a common hydrophobic binding surface [33, 34]. All known structures of HPt proteins share a characteristic 4-helix bundle with a hydrophobic binding surface for RR binding [35,36,37,38,39,40,41,42]. The phosphorylatable histidine residue is located on the periphery of this hydrophobic patch on the αC helix of the 4-helix bundle and is completely solvent-exposed [1, 35, 41].
Despite their remarkably similar tertiary structure, HPt domains exhibit high sequence diversity. However, much of the αC helix and positions flanking the phosphorylatable histidine show moderate sequence conservation. These residues are often involved in maintaining structural integrity of the HPt protein or in forming intermolecular interactions with binding partners. Intramolecular interactions of conserved residues N61 and K67 of Ypd1 help stabilize the 4-helix bundle and pull the side chains away from the phospho-accepting histidine (H64). This ensures accessibility of the phosphoryl group for cognate response regulators [39, 41, 43]. In the BeF3− bound complex of Ypd1 and Sln1-R1, the side chains of the Ypd1 K67 and R90 residues are involved in intermolecular interactions with the receiver domain [44, 45]. A glycine located four residues from the phosphorylatable histidine (H + 4) has been shown to be involved in protein-protein interactions and/or phosphoryl transfer in both yeast and bacteria [33, 45,46,47,48]. Previous results using a yeast two-hybrid assay indicated that substitution of a glutamine at the H + 4 position in S. cerevisiae Ypd1(G68Q) may impair interactions with the receiver domains of its cognate RRs . The ability of Ypd1-G68Q to both accept and transfer phosphoryl groups was also shown to be diminished [45, 46]. Further kinetic studies indicated that despite a dramatic decrease in the rate of phosphoryl transfer between Sln1-R1 and Ypd1-G68Q, binding affinity remained similar to wild-type (WT) . We hypothesized that the glutamine substitution at residue 68 resulted in a catalytic defect rather than a significant change in protein binding affinity.
Here we report a comprehensive analysis of a more extensive set of substitutions at position 68 of Ypd1 to gain further insight into the evolutionary constraints leading to the unusually high conservation of glycine at this position. We combine bioinformatics, radio-isotopic phosphoryl transfer assays, X-ray crystallography, fluorescence-based binding data and molecular modelling techniques to highlight the importance of key intermolecular interactions required for optimal phosphotransfer between an HPt protein and its cognate RR.
Residues in the H + 4 position of HPt domains
Approximately 10,000 non-redundant sequences, representing bacteria, fungi, and plant HPt sequences obtained from the Pfam database , were analyzed to determine what percentage of residues were found in the H + 4 position. Figure 1 shows the sequence alignment of the predicted αC and αD helices of the core 4-helix bundle from a representative set of HPt proteins and a WebLogo created using the complete alignment showing the frequency of each residue. The H + 4 position is highly conserved throughout all sequences analyzed. Glycine was found in the H + 4 position in approximately 87% of the sequences that were aligned, with approximately 10% of sequences having serine in the H + 4 position (Table 1).
Non-conservative substitutions at the H + 4 position disrupt phosphotransfer
Various amino acid residues (S, A, V, L, E, Q) were introduced to the G68 position of Ypd1 in order to analyze what effects amino acids other than glycine have on the phosphorelay activity of Ypd1. Phosphorelay experiments were performed using each of the Ypd1-G68X substituted proteins with the receiver domain of the upstream binding partner (Sln1-R1) as a donor and the receiver domain of the downstream binding partner (Ssk1-R2) as a recipient. Ypd1-G68S and Ypd1-G68A both accepted phosphoryl groups from Sln1-R1 at approximately the same level as wild-type Ypd1 (Table 2, Fig. 2). Ypd1-G68Q showed significantly decreased phosphorylation (~ 40% of wild-type) while Ypd1-G68 V, Ypd1-G68 L and Ypd1-G68E were severely impaired in accepting phosphoryl groups (less than 3% of wild-type) (Table 2, Fig. 2). In phosphorelay experiments (transfer from Sln1-R1 to Ypd1-G68X to Ssk1-R2) Ypd1-G68S and Ypd1-G68A exhibited phosphorelay activity at levels of ~ 80% to that of wild-type Ypd1. In contrast, Ypd1-G68Q showed severely impaired phosphorelay to Ssk1-R2 (Fig. 3), consistent with previously published results . Due to their inability to accept phosphoryl groups from Sln1-R1, no phosphotransfer was observed from Ypd1-G68V, Ypd1-G68L or Ypd1-G68E to Ssk1-R2.
Substitutions at the H + 4 position cause only modest changes in binding affinity
A fluorescence-based in vitro binding assay was developed to gain insight into the differences in binding between Ypd1 and its partners. A substitution was made on Ypd1 (T12) adjacent to the hydrophobic binding patch (but in close proximity of the active site) to introduce a unique, solvent exposed cysteine. This cysteine was used for thiol-specific labelling with a fluorescent probe, 5-iodoacetamidofluorescein (5-IAF). Ypd1-T12C~F functions in vitro in phosphotransfer assays similarly to wild-type Ypd1 (data not shown). The titration of 5-IAF labelled Ypd1 with Sln1-R1 increased fluorescence intensity above baseline buffer dilutions, resulting in binding curves that appear to reach saturation (Fig. 4). Observed equilibrium dissociation constants (Kd), calculated from these binding curves for this panel of mutant proteins, ranged from 0.5 to 3 μM as shown in Table 3. The observed Kd for the Sln1-R1 and Ypd1-T12C interaction, 0.94 ± 0.38 μM, is in agreement with the observed Kd between Sln1-R1 and wild-type Ypd1 calculated from published kinetics data [46, 50]. Though the estimated Kd values for the mutants were within the error of the Kd observed for wild-type Ypd1, substitutions with hydrophobic side chains showed a slight increase in Kd while hydrophilic side chains showed the opposite trend (Table 3).
Structural integrity of the Ypd1 G68X mutants
The X-ray structure of the Ypd1-G68Q mutant was determined in order to ascertain structural integrity of the mutant and to gain insight into its loss of function characteristics. The Ypd1-G68Q mutant protein crystallized in space group P3121. The structure was solved to a resolution of 1.98 Å using molecular replacement. The model contains residues 2–167 with an average B-factor of 23.73 Å2. X-ray data collection and refinement statistics are presented in Table 4. Clear electron density was observed for the side chain of the glutamine substitution at position 68 (see inset of Fig. 5). The root mean square deviation (RMSD) for all residues between the Ypd1-G68Q and wild type structure is 1.9 Å. Few differences are apparent when comparing this structure and the previously reported Ypd1 crystal structure (PDB ID: 1QSP), Figs. 5 and 6 [35, 44, 51]. The area around the site of phosphorylation is unperturbed with an RMSD of 0.2 Å for all residues in αC and αD helix. The N-terminal αA helix and the following turn (residues 11–21) show the largest shifts in the C-alpha positions with an RMSD of 1.7 Å. The αB helix is extended by one turn (residues 22–26) in the Ypd1-G68Q structure. The αA helix rotates approximately 30° around an axis at its N-terminus and αA helix makes a ¼ rotation around its longitudinal axis (Fig. 5). Upon the αA twisting movement, the originally exposed I13 and I17 become buried, while L14 and I18 are now exposed. Thus, hydrophobic interactions between αA and the rest 4-helix bundle are maintained, but by different residues. Minor shifts in the orientations of exposed side chains account for the remainder of the deviation between Ypd1 structures. The crystal structure was also determined for Ypd1-G68E (non-functional). The structure showed little overall change in comparison to wild-type Ypd1 (data not shown). In order to assess structural integrity of other Ypd1 variants, Fourier-transform infrared spectroscopy (FTIR) data were collected for wild-type Ypd1, Ypd1-G68S (functional) and Ypd1-G68L (non-functional). Despite some sample-to-sample variation, the FTIR spectra of tested Ypd1 variants were consistent with the observed well-folded α-helical nature of HPt proteins (data not shown).
Molecular modelling of H + 4 substitutions
To further explain the effects of the H + 4 residue substitutions in Ypd1, residues were modelled onto the existing Sln1-R1/Ypd1-BeF3− structure (PDB ID: 2R25). Brief energy minimization and relaxation steps were performed on the mutant active sites to remove clashes and estimate possible localized perturbations caused by each substitution. The following Ypd1-G68 variants were tested, in addition to a wild-type control: S, V, E, L and Q. The wild-type Ypd1 model showed little structural perturbation upon relaxation, largely preserving the original phosphoryl alignment and interaction network. Ypd1-G68L also exhibited relatively little perturbation, though the leucine side chain was arranged such as to hinder movement of the highly conserved K1195 (see Additional file 1: Figure S1 for active site models of Ypd1-G68X mutant proteins in complex with P~Sln1-R1). The Ypd1-G68V model suggested distortion of the phosphoryl alignment, increasing the distance between A1174 on the β4α4 loop of Sln1-R1 and the closest phosphoryl oxygen. Like in Ypd1-G68L, the substituted valine side chain was oriented towards K1195 in Sln1. The Ypd1-G68E model exhibited similar effects and showed a larger shift in A1174 on the β4α4 loop of Sln1-R1. The positioning of the acidic side chain suggests an ability to form an intramolecular salt-bridge with K67 of Ypd1. While the Ypd1-G68S model showed an increase in the distance to A1174, the serine side chain was able to directly interact with the phosphoryl group. Finally, the Ypd1-G68Q model exhibited perturbations resembling the Ypd1-G68V model. However, despite sharing similarities with the hydrophobic substitution, the mutant Ypd1-G68Q side chain is oriented away from the phosphorylatable H64 and appeared capable of forming a hydrogen bond with residues outside the active site. The hydrophilicity of the glutamine residue, along with this reorientation, may reduce potential clashes with the K1195 side chain and allow for the low-level functionality of Ypd1-G68Q. The additional intermolecular interactions seen in the Ypd1-G68Q and Ypd1-G68E models are likely responsible for the modest increases in binding affinity observed with these mutants (Table 4). While these modelling observations support the mutant phosphotransfer data, the limitations of static structural models suggest that more extensive in silico studies are needed.
HPt proteins play critical roles in signal transduction. Their primary function is to transfer phosphoryl groups from the receiver domain of a HHK to the receiver domain of an RR protein. Bacteria and yeast with deleterious mutations of HPt genes are either inviable or exhibit decreased cell viability through suboptimal pathway regulation [9, 11, 52,53,54,55]. For example, the HPt domain of the HK-RR-HPt protein ArcB from E. coli transmits a signal to the terminal response regulator ArcA. Mutants of residues in ArcBC, notably the H + 4 residue G721, show a decrease in phosphotransfer . Similarly, substitution of the H + 4 residue (G52) of the P1 domain from CheA (an HPt domain) has a detrimental effect on chemotaxis . The Ypd1-G68Q mutant from S. cerevisiae showed significantly diminished in vitro phosphorylation from its upstream donor Sln1 and no observable phosphotransfer to the downstream acceptor Ssk1 . In this study, we aimed to investigate the role of this H + 4 residue in His-to-Asp multi-step phosphorelay systems.
Small residues are highly conserved at the H + 4 position
Because H + 4 substitutions in HPt domains result in detrimental effects in both bacteria and yeast, a comprehensive sequence alignment was performed on all protein sequences predicted to be stand-alone HPt proteins or multi-domain proteins with embedded HPt domains. Residues with small-volume side chains were found to occupy the H + 4 position in 98% of the sequences analyzed. Glycine appears in ~ 87% of cases, while ~ 10% were found to have serine and ~ 1% were found to have alanine. Such high conservation suggests that the presence of a small residue is essential for HPt domain function, including proper interaction with cognate binding partners and phosphotransfer activity.
Substitutions at the H + 4 position do not alter the overall structure of Ypd1
To test if the functional defects observed for the S. cerevisiae Ypd1-G68X substitutions were a result of loss of structural integrity, we used X-ray crystallography to determine the structure of the Ypd1-G68Q mutant. We did not observe any broad overall structural changes, with the exception of movement of the αA helix. Electron density confirmed the presence of the bulkier Gln side chain at position 68 (Figs. 5 and 6). The intrinsic flexibility of αA suggests that the observed movement is likely due to crystal packing and not a static structural alteration . A crystal structure was also determined for Ypd1-G68E, and FTIR data were collected for Ypd1-G68S and Ypd1-G68L, all of which confirmed proper folding of the proteins (data not shown). As no overall changes were observed, we hypothesized that the H + 4 glycine must be important for either phosphotransfer and/or protein-protein interactions.
Diminished function as a phosphorelay protein is not a result of impaired binding affinity
By creating a series of amino acid substitutions in the H + 4 position, we determined that substitutions of smaller residues (S, A) at the H + 4 position still allowed for phosphotransfer at near wild-type level. Substitutions introducing larger side chain volumes (V, L, E) drastically inhibited the ability of Ypd1 to serve as both an acceptor and donor of phosphoryl groups. The only exception was the Ypd1-G68Q substitution, where a large hydrophilic side chain still allowed for partial phosphotransfer activity. In vitro fluorescence-based binding experiments between Sln1-R1 and Ypd1-G68X mutants showed no substantial change in binding affinity as a consequence of the substitutions. These data demonstrate that the diminished phosphotransfer activity that was observed for the larger side chain substitutions is likely not a consequence of changes in HPt:RR binding affinity. Taken together, our results suggest that interface perturbations introduced by the non-functional mutants at position 68 are negatively affecting catalysis of the phosphotransfer reaction.
Substitutions at the G68 position perturb active site residues involved in catalysis
Our lab previously showed that there is a hydrophobic docking site on the surface of Ypd1 for all three cognate binding partners. It consists of regions of the αA, the N-terminus of αB and the C-terminus of αC helices of Ypd1 . From the crystal structures of Sln1-R1 in complex with Ypd1, we noted that the interfaces are highly complementary. The small volume of the response regulator active site cavity would not easily accommodate a bulky side chain such as G68Q in Ypd1. If this additional bulk does not inhibit binding, as our fluorescence-based binding data confirms, it must be interfering with key residues involved in the phosphotransfer reaction. When the structures of Ypd1-G68Q and Ypd1 from the BeF3− activated complex (PDB ID: 2R25) are aligned, the mutant glutamine side chain clashes with the highly conserved K1195 residue of Sln1-R1 (Fig. 7). K1195 has been implicated in the stabilization of the transition state formed during the His-Asp phosphotransfer event . Any changes to its ability to neutralize the negatively charged transition state during the reaction may have a significant effect on phosphotransfer between Sln1-R1 and Ypd1.
Molecular modelling suggests that the side chains of Ypd1-G68V and Ypd1-G68L remain in close proximity to the K1195, likely hindering its ability to move and affecting this stabilization role. Additionally, several other factors may be affected by the substitutions. Previous work found that a conserved in-line orientation is critical for the nucleophilic attack and phosphotransfer between the histidine and aspartate residues . Correct geometry is maintained for HPt proteins and their RRs by a narrow channel through which the histidine can access the aspartate. In the Sln1-R1/Ypd1 complex, this is formed by adjacent residues on both proteins, including highly conserved positions such as Q1146, T1173, A1174 and K1195 on Sln1-R1, and K67, G68 and Q86 on Ypd1. Disruption to the arrangement of these residues would adversely affect the phosphotransfer reaction. Models of the V, E and Q substitutions exhibited various levels of distortion in this arrangement. The likely explanation for this is the introduction of a large chemical group into the active site causes steric clashes, though more extensive in silico studies are needed to confirm the full effects. Clashes may affect interactions with the β4α4 loop on Sln1-R1, particularly with the G68E substitution.
Upon phosphorylation, Sln1-R1 undergoes a conformational change involving the β4α4 region. This allows for the transfer channel to form, and for T1173 (side chain) and A1174 (main chain) to hydrogen bond with the oxygen atoms on either side of the tetrahedral phosphoryl group likely serving to stabilize the negatively charged pentavalent transition state during transfer. Modelling suggests that the larger substitutions (V, E and Q) alter the interactions of this region, increasing the distance between A1174 and the flanking phosphoryl oxygen atom. While the Ypd1-G68Q and Ypd1-G68S models also exhibited this effect, the hydrogen bonding ability of the glutamine/serine side chains produce different results. The glutamine side chain in Ypd1 is oriented away from the key active site residues in Sln1. This likely makes it more favorable and/or stable than a large hydrophobic side chain within the highly charged active site, however, we cannot rule out the possibility of changes in orientation during complex formation that may not be detectable in the models. The additional hydrogen bonding ability may also explain the increase in observed binding affinity between Ypd1-G68Q and Sln1-R1. The serine side chain was able to form a hydrogen bond directly with the phosphoryl group, compensating for the alteration in bonding with A1174. This may explain why serine is the second most abundant residue found at the H + 4 position in HPt proteins.
Implications for histidine kinases
Interestingly, while both HPt and HK domains interact with receiver domains using phosphorylatable histidine residues, the strict H + 4 conservation found for HPt domains does not translate to the dimerization and histidine phosphotransfer domain (DHp) of HK proteins, even though this domain maintains a 4-α-helical bundle for interaction with receiver domains of RRs. In most HKs, a threonine or asparagine occupies the H + 4 position in the conserved H-box motif of the DHp domain [58,59,60]. The H + 4 position has also been implicated as a crucial residue for determining whether a HK will have phosphatase activity. In the osmosensor EnvZ, an H + 4 threonine was crucial for activity . Comparison of HK:RR structures HK853:RR468 (PDB ID: 3DGE) and ThkA:TrrA from Thermotoga maritima (PDB ID: 3A0R) with HPt:RR structures Sln1-R1: Ypd1 (PDB ID: 1OXB) and CheA-P1:CheY (PDB ID: 2LP4) demonstrates that the protein-protein interactions occur in different regions on the RR partner. RR proteins interact with HK proteins using primarily the β3α3/β4α4 regions, but interact with HPt proteins using the β1α1/β2α2/β3α3 regions. An altered domain orientation allows for the larger residues found near the phosphorylatable histidine on most HKs. Large residues on the surface of the HPt proteins in the H + 4 location, as we have shown through radio-isotopic phosphotransfer assays and molecular modelling, affect residues crucial for proper HPt:RR interactions and phosphotransfer. Additional structural complexes of HK:RR cognate pairs as well as HPt:RR pairs would help to further support this observation.
In this study, we created and characterized a series of residue substitutions at G68 in the S. cerevisiae HPt protein, Ypd1, to demonstrate the necessity of a small residue in this position for proper HPt function. These results help to explain the high sequence conservation observed at this position in all known HPt proteins/domains. We subsequently found that even with large, hydrophobic substitutions, the observed binding affinity between Ypd1 and its upstream partner Sln1-R1 was unaffected. The binding data suggested that diminished phosphotransfer activity was more likely due to interference in catalysis. Structural analysis using the crystal structure of the partially functional Ypd1-G68Q mutant and comparison with known crystal structures showed that the G68 substitutions could be interfering with key active site residues. We used molecular modelling to visualize the potential effects on these catalytic residues as a result of the introduction of larger side chains into the active site. These observations suggest how the larger side chains (G68V, G68L, G68E) abolish phosphotransfer, while Ypd1-G68Q is still partially functional. In summary, the presence of a highly-conserved glycine near the site of phosphorylation is sterically and mechanistically significant and essential for phosphotransfer between HPt proteins and cognate response regulator binding partners.
The full alignment of the HPt family (entry PF01627) was downloaded from the Pfam database, including sequences of both stand-alone HPt proteins and HK proteins with HPt domains . This sequence list was edited with Jalview  to remove redundancy (with a 98% identity threshold). Any sequence lacking a conserved phosphorylatable histidine was removed. The number of non-redundant sequences remaining was approximately 10,000. Sequences were sorted and counted according to the residue at the H + 4 position. Jalview was used to construct a representative sequence alignment. WebLogo3 was used to create a sequence logo from the full alignment .
Expression and protein purification
A pUC-Ypd1 plasmid was expressed in Escherichia coli and the protein was purified using ammonium sulfate precipitation, anion exchange chromatography and size exclusion chromatography, as described previously . The pUC-Ypd1 plasmid was then used as a template to create all Ypd1-G68X mutants using site-directed mutagenesis PCR. Proteins were expressed in DH5α E. coli cells and protein purification was performed similarly to wild-type Ypd1.
The YPD1 gene was also inserted into a pET21a (+) vector for expression using the T7 promotor. To covalently attach a fluorescein molecule near the active site of Ypd1, T12 was mutated to a cysteine residue (pET-Ypd1-T12C) through two-step PCR site-directed mutagenesis. The resulting plasmid was used as a template for the creation of the double mutants. Various amino acid residues (S, A, V, L, E, Q) were introduced to the G68 position. Proteins were expressed in BL21(DE3) Star cells and purified similarly to wild-type Ypd1.
The expression vector encoding the Sln1 kinase domain (GST-Sln1-HK), was kindly provided by R. Deschenes (University of South Florida). GST-Sln1-HK was expressed and purified as a glutathione S-transferase (GST) fusion protein using glutathione Sepharose 4B resin. Protein was stored and used in assays in bead-bound form, as previously described .
The receiver domain from Sln1 (Sln1-R1) and the receiver domain of Ssk1 (Ssk1-R2) were inserted into a pFJS16 vector, as previously described . These proteins were expressed in E. coli Rosetta (DE3) cells (Novagen) as a fusion protein containing C-terminal intein and chitin binding domains and were purified by chitin affinity chromatography and gel filtration, as described previously [22, 64].
Hexagonal form Ypd1-G68Q mutant crystals were grown using an initial protein concentration of 10 mg/ml equilibrated in hanging drops over a reservoir of 0.1 M sodium acetate, pH 5.0, 0.2 M ammonium acetate and 25–30% PEG 4000 (Fluka, 81,242).
X-ray data collection and processing
Data were collected at the OU Macromolecular Crystallography Lab using CuKα radiation (1.54 Å wavelength) at 100 K by flash freezing crystals in liquid N2. The data were recorded with a Dectris Pilatus P200K hybrid pixel detector using oscillations of 0.5° and processed using HKL2000 to a resolution of 1.98 Å . The space group was determined to be P3121 with unit cell parameters of a = b = 76.7 Å, c = 66.7 Å α = β = 90°, γ = 120°. One molecule was found in the asymmetric unit. Data processing and refinement statistics are presented in Table 4.
Structure solution and refinement
Molecular replacement was performed using Phaser from the Phenix suite of programs [66,67,68] to determine the initial phases for the Ypd1-G68Q structure. The structure of wild-type Ypd1 (PDB ID: 1QSP) was used as a template for molecular replacement . Refinement was done using Phenix-refine . Clear difference electron density was observed for the glutamine side chain at position 68 in an Fo-Fc electron density map. Coot  was used for model adjustments after each cycle of refinement. The final Rwork was 17.8% with an Rfree of 20.7%. Coordinates for the Ypd1-G68Q structure were deposited to the Protein Data Bank (PDB ID: 6M7W).
The Sln1-HK domain bound to glutathione-Sepharose 4B resin was phosphorylated via incubation with 0.66 μM [γ-32P]-ATP (3000 Ci/mmol) for 30 min according to previously published protocols . Unincorporated [γ-32P]-ATP was washed from phospho-Sln1-HK with 50 mM Tris-HCl, pH 8.0, 100 mM KCl, 15 mM MgCl2, 2 mM DTT, and 20% glycerol by three consecutive centrifugations (1 min at 1000 g). Sln1-R1 was added to the reaction and incubated for 5 min with phospho-Sln1-HK. Sln1-HK was removed from the reaction through gentle centrifugation, leaving only phosphorylated Sln1-R1 in solution. Phospho-Sln1-R1 was then used as a donor to phosphorylate all Ypd1 proteins. Ypd1 proteins were phosphorylated by incubation with an equimolar concentration of Sln1-R1 for 5 min. To test the ability of the Ypd1-G68X mutants to transfer the phosphoryl group to downstream binding partners, Ypd1~P was incubated with an equimolar concentration of Ssk1-R2 and an aliquot was obtained at 5 min. The reaction was quenched with stop buffer containing EDTA and samples were separated on a 15% SDS polyacrylamide gel and electrophoresed at 200 V for 45 min for visualization. The SDS gels were wrapped in plastic wrap and exposed to a phosphorimager screen. The radioactivity of each band was quantified using a Typhoon phosphorimager (Molecular Dynamics). Band intensities were quantified using ImageJ .
Fluorescence binding assay
A substitution was made to Ypd1-T12 to introduce a unique, solvent-exposed cysteine for thiol-specific labelling with a fluorescent probe. Purified Ypd1-T12C and Ypd1-T12C-G68X mutants were buffer-exchanged into 50 mM potassium phosphate, pH 9.0 and 1 mM β-mercaptoethanol. Proteins were incubated in darkness for 2 h at room temperature with a 7-fold molar excess of 5-IAF for covalent labelling of Ypd1-T12C. Unincorporated 5-IAF was removed by exchanging labelled Ypd1 proteins into 20 mM Tris, pH 8.0, 50 mM NaCl and 10 mM MgCl2 using a GE HiTrap desalting column. The concentration of fluorescein bound to protein was estimated by absorption at 492 nm, and protein concentration was estimated by BioRad protein assay revealing that 70–90% of the Ypd1 molecules were labelled. Fluorescently-labelled proteins were aliquoted and stored in the presence of 10% glycerol at − 20 °C.
The Sln1-R1 receiver domain was purified as described previously, however, fluorescence reaction buffer (20 mM Tris, pH 8.0, 50 mM NaCl and 10 mM MgCl2) was substituted during size exclusion chromatography. Chelex® resin (BioRad) was used to strip contaminating cations from the Tris-salt solution before magnesium chloride was added to the buffer.
Binding of Sln1-R1 to fluorescein labelled Ypd1-T12C induces a change in the fluorescein moiety resulting in altered fluorescence intensity. A Fluoromax 4 Spectrofluorometer from Horiba Scientific, temperature controlled to 23.0 °C, was used to observe changes in fluorescence caused by binding. IAF-labelled Ypd1-T12C (30 pmol) was diluted to 1.9 mL in fluorescence reaction buffer, and Sln1-R1 was titrated into the reaction such that the concentration in the cuvette ranged from 10 nM to 6 μM. Upon addition of Sln1-R1, the solution was mixed with a magnetic stir bar for 30 s and allowed to rest for an additional 20 s before reading fluorescence intensity with absorbance at 492 nm and emission at 515 nm. Intensity after each addition (F) as a fraction of intensity from labelled Ypd1 alone (F0) was calculated for titration with Sln1-R1 and buffer alone. The difference between these two normalized intensities (F/F0, Sln1-R1 – F/F0, buffer) indicates binding of Sln1-R1 to labelled Ypd1. Plotting change in fluorescence intensity caused by Sln1-R1 versus concentration of Sln1-R1 shows a binding curve with saturation at high concentrations. These curves were fitted using Mathematica  to an expanded quadratic equation with parameters accounting for fluorescence from both the bound and unbound states of Ypd1 and the dissociation constant for the Ypd1:Sln1-R1 complex was calculated. The average dissociation constant and standard deviation of the mean are reported here.
Ypd1-G68X substitutions were modelled initially in PyMOL. For Ypd1-G68Q and Ypd1-G68E (unpublished data), crystal structures were aligned to the existing Sln1-R1/Ypd1-BeF3− complex (PDB ID: 2R25). The mutant Ypd1 and Sln1-R1 molecules were extracted for brief energy minimization and relaxation. For the remaining substitutions, residues were modelled directly into the active site of the Sln1-R1/Ypd1-BeF3− structure. In each model, the BeF3− ligand atoms were replaced with a phosphoryl group. Each system was stripped of crystallographic waters and ligands, with only the Mg2+ cation being retained. Structures were then re-solvated in an orthorhombic solvent box with 10 Å padding using the TIP3P solvent model . Finally, systems were neutralized and ionized to a concentration of 0.15 M NaCl. System preparation was done using the Maestro graphic user interface from the Schrödinger molecular modelling suite (2016–1 release) . Runs were performed in the Desmond molecular dynamics software package using the OPLS_2005 force field through the Maestro interface (released with the Schrödinger suite) [75, 76]. The default Desmond relaxation protocol was used, featuring two rounds of minimization, followed by a series of gradually diminishing restraints over ~ 160 ps and a brief, 100 ps unrestrained segment at constant temperature and pressure of 300 K and 1.013 bar, respectively. Snapshots were aligned by Cα atoms and averaged over the last 100 ps to generate representative models. The minimized and relaxed active site models were then visualized in PyMOL .
All molecular figures were generated using PyMOL .
Dimerization and histidine phosphotransfer domain
Fourier-transform infrared spectroscopy
Hybrid Histidine Kinase
High Osmolarity Glycerol
Histidine Phosphotransfer protein (or domain)
Mitogen-Activated Protein Kinase
Root Mean Square Deviation
Receiver domain of Sln1
Receiver domain of Ssk1
Fassler JS, West AH. Histidine phosphotransfer proteins in fungal two-component signal transduction pathways. Euk Cell. 2013;12(8):1052–60.
Stock AM, Robinson VL, Goudreau PN. Two-component signal transduction. Annu Rev Biochem. 2000;69:183–215.
Saito H. Histidine phosphorylation and two-component signaling in eukaryotic cells. Chem Rev. 2001;101:2497–509.
D'Agostino IB, Kieber JJ. Phosphorelay signal transduction: the emerging family of plant response regulators. Trends Biochem Sci. 1999;24(Nov.):452–6.
Tsuzuki M, Ishige K, Mizuno T. Phosphotransfer circuitry of the putative multi-signal transducer, ArcB, of Escherichia coli: in vitro studies with mutants. Mol Microbiol. 1995;18:953–62.
Bilwes AM, Alex LA, Crane BR, Simon MI. Structure of CheA, a signal-transducing histidine kinase. Cell. 1999;96(Jan. 8):131–41.
Freeman JA, Bassler BL. Sequence and function of LuxU: a two-component phosphorelay protein that regulates quorum sensing in Vibrio harveyi. J Bacteriol. 1999;181(3):899–906.
Calera JA, Herman D, Calderone R. Identification of YPD1, a gene of Candida albicans which encodes a two-component phosphohistidine intermediate protein. Yeast. 2000;16:1053–9.
Lee JW, Ko YJ, Kim SY, Bahn YS. Multiple roles of Ypd1 phosphotransfer protein in viability, stress response, and virulence factor regulation in Cryptococcus neoformans. Euk Cell. 2011;10(7):998–1002.
Miyata S, Urao T, Yamaguchi-Shinozaki K, Shinozaki K. Characterization of genes for two-component phosphorelay mediators with a single HPt domain in Arabidopsis thaliana. FEBS Lett. 1998;437:11–4.
Posas F, Wurgler-Murphy SM, Maeda T, Witten EA, Thai TC, Saito H. Yeast HOG1 MAP kinase cascade is regulated by a multistep phosphorelay mechanism in the SLN1-YPD1-SSK1 "two-component" osmosensor. Cell. 1996;86:865–75.
Tamás MJ, Rep M, Thevelein JM, Hohmann S. Stimulation of the yeast high osmolarity glycerol (HOG) pathway: evidence for a signal generated by a change in turgor rather than by water stress. FEBS Lett. 2000;472:159–65.
Bhate MP, Molnar KS, Goulian M, DeGrado WF. Signal transduction in histidine kinases: insights from new structures. Structure. 2015;23(6):981–94.
Diensthuber RP, Bommer M, Gleichmann T, Möglich A. Full-length structure of a sensor histidine kinase pinpoints coaxial coiled coils as signal transducers and modulators. Structure. 2013;21(July 2):1127–36.
Gao R, Stock AM. Biological insights from structures of two-component proteins. Annu Rev Microbiol. 2009;63:133–54.
Appleby JL, Parkinson JS, Bourret RB. Signal transduction via the multi-step phosphorelay: not necessarily a road less traveled. Cell. 1996;86:845–8.
Saito H, Posas F. Response to hyperosmotic stress. Genetics. 2012;192(Oct.):289–318.
Levin DE. Cell wall integrity signaling in Saccharomyces cerevisiae. Microbiol Mol Biol Rev. 2005;69(2):262–91.
Fassler J, West AH. Genetic and biochemical analysis of the SLN1 pathway in Saccharomyces cerevisiae. Meth Enzymol. 2010;471:291–317.
Hohmann S. Osmotic stress signaling and osmoadaptation in yeasts. Microbiol Mol Biol Rev. 2002;66(2):300–72.
Posas F, Saito H. Activation of the yeast SSK2 MAP kinase kinase kinase by the SSK1 two-component response regulator. EMBO J. 1998;17(5):1385–94.
Li S, Ault A, Malone CL, Raitt D, Dean S, Johnston LH, et al. The yeast histidine protein kinase, Sln1p, mediates phosphotransfer to two response regulators, Ssk1p and Skn7p. EMBO J. 1998;17(23):6952–62.
Cherry JM, Hong EL, Amundsen C, Balakrishnan R, Binkley G, Chan ET, et al. Saccharomyces genome database: the genomics resource of budding yeast. Nucleic Acids Res. 2011;40(D1):D700–D5.
Fassler JS, West AH. Fungal Skn7 stress responses and their relationship to virulence. Euk Cell. 2011;10(2):156–67.
Li S, Dean S, Li Z, Horecka J, Deschenes RJ, Fassler JS. The eukaryotic two-component histidine kinase Sln1p regulates OCH1 via the transcription factor, Skn7p. Mol Biol Cell. 2002;13(Feb.):412–24.
Lu JM-Y, Deschenes RJ, Fassler JS. Saccharomyces cerevisiae histidine phosphotransferase Ypd1p shuttles between the nucleus and cytoplasm for SLN1-dependent phosphorylation of Ssk1p and Skn7p. Euk Cell. 2003;2(6):1304–14.
Maeda T, Wurgler-Murphy SM, Saito H. A two-component system that regulates an osmosensing MAP kinase cascade in yeast. Nature. 1994;369:242–5.
Kaserer AO, Andi B, Cook PF, West AH. Kinetic measurements for studying phosphorelay signaling. Meth Enzymol. 2010;471:291–317.
Tamás MJ, Luyten K, Sutherland FCW, Hernandez A, Albertyn J, Valadi H, et al. Fps1p controls the accumulation and release of the compatible solute glycerol in yeast osmoregulation. Mol Microbiol. 1999;31(4):1087–104.
Capaldi AP, Kaplan T, Liu Y, Habib N, Regev A, Friedman N, et al. Structure and function of a transcriptional network activated by the MAPK Hog1. Nature Genet. 2008;40(11):1300–6.
Albertyn J, Hohmann S, Thevelein JM, Prior BA. GPD1, which encodes glycerol-3-phosphate dehydrogenase, is essential for growth under osmotic stress in Saccharomyces cerevisiae, and its expression is regulated by the high-osmolarity glycerol response pathway. Mol Cell Biol. 1994;14(6):4135–44.
Ota IM, Varshavsky A. A gene encoding a putative tyrosine phosphatase suppresses lethality of an N-end rule-dependent mutant. Proc Natl Acad Sci U S A. 1992;89:2355–9.
Porter SW, West AH. A common docking site for response regulators on the yeast phosphorelay protein YPD1. Biochim Biophys Acta. 2005;1748:138–45.
Porter SW, Xu Q, West AH. Ssk1p response regulator binding surface on histidine-containing phosphotransfer protein Ypd1p. Euk Cell. 2003;2(1):27–33.
Xu Q, West AH. Conservation of structure and function among histidine-containing phosphotransfer (HPt) domains as revealed by the crystal structure of YPD1. J Mol Biol. 1999;292:1039–50.
Sugawara H, Kawano Y, Hatakeyama T, Yamaya T, Kamiya N, Sakakibara H. Crystal structure of the histidine-containing phosphotransfer protein ZmHP2 from maize. Protein Sci. 2006;14:202–8.
Kato M, Mizuno T, Shimizu T, Hakoshima T. Refined structure of the histidine-containing phosphotransfer (HPt) domain of the anaerobic sensor kinase ArcB from Escherichia coli at 1.57 Å resolution. Acta Cryst. 1999;D55:1842–9.
Ulrich DL, Kojetin D, Bassler BL, Cavanagh J, Loria JP. Solution structure and dynamics of LuxU from Vibrio harveyi, a phosphotransferase protein involved in bacterial quorum sensing. J Mol Biol. 2005;347:297–307.
Ruszkowski M, Brzezinski K, Jedrzejczak R, Dauter M, Dauter Z, Sikorski M, et al. Medicago truncatula histidine-containing phosphotransfer protein: structural and biochemical insights into the cytokinin transduction pathway in plants. FEBS J. 2013;280:3709–20.
Rogov VV, Bernhard F, Lohr F, Dotsch V. Solution structure of the Escherichia coli YojN histidine-phosphotransferase domain and its interaction with cognate phosphoryl receiver domains. J Mol Biol. 2004;343:1035–48.
Xu Q, Carlton D, Miller MD, Elsliger M-A, Krishna SS, Abdubek P, et al. The crystal structureof a histidine phosphotransfer protein ShpA, an essential regulator of stalk biogenesis in Caulobacter cresentus. J Mol Biol. 2009;390:686–98.
Bauer J, Reiss K, Veerabagu M, Heunemann M, Harter K, Stehle T. Structure-function analysis of Arabidopsis thaliana histidine kinase AHK5 bound to its cognate phosphotransfer protein AHP1. Mol Plant. 2012;6(3):959–70.
Xu Q, Nguyen V, West AH. Purification, crystallization, and preliminary X-ray diffraction analysis of the yeast phosphorelay protein YPD1. Acta Cryst. 1999;D55:291–3.
Zhao X, Copeland DM, Soares AS, West AH. Crystal structure of a complex between the phosphorelay protein YPD1 and the response regulator domain of SLN1 bound to a phosphoryl analog. J Mol Biol. 2008;375(4):1141–51.
Janiak-Spens F, West AH. Functional roles of conserved amino acid residues surrounding the phosphorylatable histidine of the yeast phosphorelay protein YPD1. Mol Microbiol. 2000;37(1):136–44.
Janiak-Spens F, Cook PF, West AH. Kinetic analysis of YPD1-dependent phosphotransfer reactions in the yeast osmoregulatory phosphorelay system. Biochemistry. 2005;44(1):377–86.
Matsushika A, Mizuno T. The structure and function of the histidine-containing phosphotransfer (HPt) signaling domain of the Escherichia coli ArcB sensor. J Biochem. 1998;124:440–5.
Nakamura A, Kakimoto T, Imamura A, Suzuki T, Ueguchi C, Mizuno T. Biochemical characterization of a putative cytokinin-responsive his-kinase, CKI1, from Arabidopsis thaliana. Biosci Biotechnol Biochem. 1999;63(9):1627–30.
Finn RD, Coggill P, Eberhardt RY, Eddy SR, Mistry J, Mitchell AL, et al. The Pfam protein families database: towards a more sustainable future. Nucleic Acids Res. 2016;44(D1):279–85.
Stojanovski K, Ferrar T, Benisty H, Uschner F, Delgado J, Jimenez J, et al. Interaction dynamics determine signaling and output pathway responses. Cell Rep. 2017;19(April 4, 2017):136–49.
Xu Q, Porter SW, West AH. The yeast YPD1/SLN1 complex: insights into molecular recognition in two-component systems. Structure. 2003;11(Dec. 2003):1569–81.
Biondi EG, Skerker JM, Arif M, Prasol MS, Perchuck BS, Laub MT. A phosphorelay system controls stalk biogenesis during cell cycle progression in Caulobacter cresentus. Mol Microbiol. 2006;59(2):386–401.
Bahn Y-S, Kojima K, Cox GM, Heitman J. A unique fungal two-component system regulates stress responses, drug sensitivity, sexual development, and virulence of Cryptococcus neoformans. Mol Biol Cell. 2006;17(July):3122–35.
Hsu J-L, Chen H-C, Peng H-L, Chang H-Y. Characterization of the histidine-containing phosphotransfer protein B-mediated multistep phosphorelay system in Pseudomonas aeruginosa PAO1. J Biol Chem. 2008;283(15):9933–44.
Mavrianos J, Desai C, Chauhan N. Two-component histidine phosphotransfer protein Ypd1 is not essential for viability in Candida albicans. Euk Cell. 2014;13(4):452–60.
Schuster M, Silversmith RE, Bourret RB. Conformational coupling in the chemotaxis response regulator CheY. Proc Natl Acad Sci U S A. 2001;98(11):6003–8.
Herschlag D, Jencks WP. The effects of Mg2+, hydrogen bonding, and steric factors on rate and equilibrium constants for phosphoryl transfer between carboxylate ions and pyridines. J Am Chem Soc. 1990;112(5):1942–50.
Stock J, Levit MN, Wolanin PM. Information processing in bacterial chemotaxis. Science's STKE. 2002;https://stke.sciencemag.org/content/2002/132/pe25.
Grebe TW, Stock JB. The histidine protein kinase superfamily. Adv Micro Physiol. 1999;41:139–227.
Kim D-J, Forst S. Genomic analysis of the histidine kinase family in bacteria and archaea. Microbiology. 2001;147:1197–212.
Dutta R, Yoshida T, Inouye M. The critical role of the conserved Thr247 residue in the functioning of the osmosensor EnvZ, a histidine kinase/phosphatase, in Escherichia coli. J Biol Chem. 2000;275(49):38645–53.
Waterhouse AM, Procter JB, Martin DM, Clamp M, Barton GJ. Jalview version 2—a multiple sequence alignment editor and analysis workbench. Bioinformatics. 2009;25(9):1189–91.
Crooks GE, Hon G, Chandonia J-M, Brenner SE. WebLogo: a sequence logo generator. Genome Res. 2004;14(6):1188–90.
Janiak-Spens F, Sparling JM, Gurfinkel M, West AH. Differential stabilities of phosphorylated response regulator domains reflect functional roles of the yeast osmoregulatory SLN1 and SSK1 proteins. J Bacteriol. 1999;181(2):411–7.
Otwinowski Z, Minor W. Processing of X-ray diffraction data collected in oscillation mode. Methods Enzymol. 1997;276:307–26.
Adams PD, Afonine PV, Bunkoczi G, Chen VB, Davis IW, Echols N, et al. PHENIX: a comprehensive python-based system for macromolecular structure solution. Acta Cryst. 2010;D66:213–21.
McCoy AJ, Grosse-Kunstieve RW, Adams PD, Winn MD, Storoni LC, Read RJ. Phaser crystallographic software. J Appl Crystallogr. 2007;40:658–74.
Terwilliger TC, Grosse-Kunstleve RW, Afonine PV, Moriarty NW, Zwart PH, Hung L-W, et al. Iterative model building, structure refinement and density modification with the PHENIX AutoBuild wizard. Acta Crystallogr D Biol Crystallogr. 2008;64(1):61–9.
Afonine PV, Grosse-Kunstleve RW, Echols N, Headd JJ, Moriarty NW, Mustyakimov M, et al. Towards automated crystallographic structure refinement with phenix. Refine. Acta Crystallogr D Biol Crystallogr. 2012;68(4):352–67.
Emsley P, Cowtan K. Coot: model-building tools for molecular graphics. Acta Crystallogr. 2004;D 60:2126–32.
Rasband W, Image J. US national institutes of health. Maryland: Bethesda; 1997.
Wolfram S. Wolfram research. Inc, Mathematica, Version. 2013;8:23.
Jorgensen WL, Chandrasekhar J, Madura JD. Comparison of simple potential functions for simulating liquid water. J Chem Phys. 1983;79(2):926–35.
Release S. 2: Maestro, version 9.8. Schrödinger, LLC, New York, NY. 2014.
Banks JL, Beard HS, Cao Y, Cho AE, Damm W, Farid R, et al. Integrated modeling program, applied chemical theory (IMPACT). J Comput Chem. 2005;26(16):1752–80.
Bowers KJ, Chow E, Xu H, Dror RO, Eastwood MP, Gregersen BA, et al., editors. Scalable algorithms for molecular dynamics simulations on commodity clusters. SC 2006 Conference, Proceedings of the ACM/IEEE; 2006: IEEE.
DeLano WL. The PyMOL molecular graphics system. San Carlos: DeLano Scientific; 2002.
Karplus PA, Diederichs K. Linking crystallographic model and data quality. Science. 2012;336(6084):1030–3.
We are grateful for the helpful discussions with P. Sims and P.F. Cook. We thank C. Bourne for use of the Horiba spectrofluorometer. K. Branscum for help in preparation and reading of the manuscript, and K. Soni for his assistance with some of the X-ray data collection and analysis.
This work was supported by grants from the National Science Foundation (MCB 1158319) and the Oklahoma Center for the Advancement of Science and Technology (HR12–059). The OU Macromolecular Crystallography Laboratory was supported by an Institutional Development Award from the National Institute of General Medical Sciences of the National Institutes of Health under grant number P20GM103640.
Availability of data and materials
The atomic coordinates and structure factor amplitudes are available in the Protein Data Bank repository PDB ID: 6M7W. Sequence alignment and molecular dynamics data are available on request.
The authors declare that they have no competing interests.
Springer Nature remains neutral with regard to jurisdictional claims in published maps and institutional affiliations.
Figure S1. Average active site models for Ypd1-G68X variants. Representative active sites calculated by averaging the last 100 unrestrained ps following energy minimization and relaxation. G68X substitutions are labelled, depicted in red spheres. The phosphoryl group and conserved active site residues are depicted in stick representation. The first panel depicts the BeF3− activated complex of Sln1-R1 and wild-type Ypd1 (PDB ID: 2R25) with BeF3− depicted in stick representation. (TIF 4327 kb)
About this article
Cite this article
Kennedy, E.N., Hebdon, S.D., Menon, S.K. et al. Role of the highly conserved G68 residue in the yeast phosphorelay protein Ypd1: implications for interactions between histidine phosphotransfer (HPt) and response regulator proteins. BMC Biochem 20, 1 (2019). https://doi.org/10.1186/s12858-019-0104-5
- Two-component signal transduction
- HPt proteins
- Response regulator
- Protein-protein interactions
- Evolutionary conservation