Diacylglycerol kinase catalyses the ATP-dependent conversion of diacylglycerol to phosphatidic acid in the plasma membrane of Escherichia coli. The small size of this integral membrane trimer, which has 121 residues per subunit, means that available protein must be used economically to craft three catalytic and substrate-binding sites centred about the membrane/cytosol interface. How nature has accomplished this extraordinary feat is revealed here in a crystal structure of the kinase captured as a ternary complex with bound lipid substrate and an ATP analogue. Residues, identified as essential for activity by mutagenesis, decorate the active site and are rationalized by the ternary structure. The γ-phosphate of the ATP analogue is positioned for direct transfer to the primary hydroxyl of the lipid whose acyl chain is in the membrane. A catalytic mechanism for this unique enzyme is proposed. The active site architecture shows clear evidence of having arisen by convergent evolution.
Diacylglycerol kinase (DgkA) is the smallest known kinase. In Escherichia coli, it is responsible for the adenosine triphosphate (ATP)-dependent phosphorylation of diacylglycerol (DAG) to phosphatidic acid used in periplasm membrane-derived oligosaccharide synthesis in response to osmotic shock1. The enzyme has long served as a model for integral membrane enzymology1,2,3, folding4,5,6, assembly7,8,9 and stability10,11. It is a trimer with three active sites of the shared sites type that exhibits moderate positive heteroallostery, random-binding kinetics and lipid substrate promiscuity1.
High-resolution X-ray structures of wild-type (WT) and functional thermostable mutants (Δ4, Δ7) of DgkA were obtained using protein crystallized in a membrane environment by the lipid cubic phase (LCP) or in meso method12. In contrast to a solution NMR structure that displayed domain swapping13, the crystallized kinase showed a simple quaternary arrangement in which adjacent monomers created shared active sites. Considerable effort was devoted to demonstrating that the enzyme was functionally active in the crystal12. While the model included a lipid substrate, a monoacylglycerol (7.8 MAG), its functional relevance remained uncertain in the absence of a nucleotide bound structure. Here we report such a structure, along with mutagenesis studies, molecular dynamics simulations (MDS) and density functional theory (DFT) modelling, which explain a wealth of biochemical and biophysical data and support a mechanism for direct transphosphorylation by this diminutive kinase.
Crystallization and overall structure
Because DgkA was crystallized in the LCP composed of MAGs (ref. 14), which double as lipid substrates15, solving a structure with ATP bound was impossible – the enzyme turns over catalytically as soon as nucleotide is added. Therefore, the enzyme was co-crystallized with the non-hydrolysable ATP analogue, adenylylmethylenediphosphonate (ACP). Producing structure-grade crystals of the complex involved extensive screening of protein constructs and crystallization conditions including host lipid MAGs. Best crystals, providing a ternary complex structure with ACP and lipid bound at 2.7 Å resolution (Table 1), were obtained with Δ4-DgkA grown in 9.9 MAG at 4 °C and soaked with zinc-ACP.
Like the apo-enzyme12, the ternary complex is a homo-trimer (Fig. 1a,b). Each subunit has four helices, three of which are largely membrane embedded (H1-3), whereas the fourth, an N-terminal amphiphilic surface helix (SH), anchors the protein at the membrane interface (Supplementary Fig. 1a). Stereo images of individual subunit models and the electron density on which the models are based are shown in Supplementary Fig. 2. H2 and H3 extend out of the membrane and are connected by a cytosolic loop (CL) whose conformation and sequence position in the protein differ between subunits in ways that may have functional consequences (Supplementary Fig. 3), as discussed below. Individual subunits are identified suA, suB and suC. The trimer has three active sites of the shared sites type. Each site has contributions from two subunits, identified asAB, asBC and asCA, where asAB is created by the SH of suA and H1-3 of suB. In the complex, asBC has zinc-ACP and lipid bound (Fig. 1a,b). The other two sites are nucleotide-free.
Ternary complex structure
The ternary complex site, asBC, contains zinc-ACP and two lipid substrates (Fig. 1a). The zinc-ACP is close to fully extended and is secured by electrostatic, hydrogen bonding and hydrophobic interactions along its length on the relatively flat, cytosol-exposed surface of H2C and H3C (Fig. 1a,c,d). The enzyme has a requirement for metal ions, known to be satisfied by zinc16. The two zinc atoms (Zn1, Zn2) bound to ACP were identified and positioned in the complex by anomalous scattering (Fig. 1e). They are bidentately coordinated, respectively, by the β- and γ- and the α- and γ-phosphates of ACP and fasten the polyphosphate to conserved residues Glu28C and Glu76C (Supplementary Table 1 and Supplementary Fig. 1b) in the active site in ways that make catalytic sense (Fig. 2a). MDS illustrate interactions between the γ-phosphate and the backbone amides of Ala29C and Ala30C (Supplementary Movie 1), both of which contribute to the helix dipole of H1C.
The two hydroxyls of ribose in ACP are tightly hydrogen bonded to the side-chain carboxyl of the essential Asp95C (Fig. 3a). These contribute to substrate binding and specificity, and explain why 2′-deoxy-ATP, with one less hydroxyl anchor to the protein, is a considerably poorer substrate2. Hydrophobic interactions between the non-polar surface of the ribose and the methylenes of Lys94C, itself a critical residue9,13 (Fig. 2b), contribute to fixing the ribose in place and to having it correctly oriented (Fig. 3a).
The purine ring of ACP is locked in position by hydrogen bonds between the N1 and N6 of adenine and the backbone linkage of His87C and Glu85C, respectively, in CLC (Fig. 3a). Such backbone-adenine interactions form the basis of nucleotide recognition by analogy with base pairing in nucleic acids. Backbone interactions are relatively residue non-specific. This explains mutagenesis work where neither residue was identified as essential (Fig. 2b and Supplementary Table 1). Between Glu85 and His87 is Tyr86C whose tyrosyl ring hovers close to the adenyl of ACP poised for π–π stacking to lock adenine firmly against the protein (Supplementary Fig. 3c,f). We refer to these three sequential residues as the clamping triad. The purine is secured too by its N7 interaction with the ɛ-amino of Lys94C, which also interacts with the α-phosphate of ATP, and is tethered in place by a salt bridge with Asp80C (Fig. 3a). As expected, this position is, by contrast, sensitive to mutation. Together with Glu85C, His87C and Asp95C, Lys94C acts like a multiply tipped pincer to lock the adenosine of ACP in a specific orientation on the protein (Fig. 3a). Measured kcat values of DgkA for guanosine triphosphate (GTP) and inosine triphosphate (ITP) are reduced by orders of magnitude compared with ATP (ref. 2). This purine selectivity makes sense in light of the ternary structure. Thus, replacing the N6 in adenine with an O6 in guanine or inosine would lead to unfavourable interactions between the two purines and adjacent backbone carbonyls of Gly83, Ser84, Glu85 and Val79. Clear evidence of instability with GTP was observed by MDS. Likewise, the crystal structure is not compatible with tight pyrimidine nucleotide binding, consistent with the observation that while adenine nucleotides dissolved crystals of DgkA, cytidine triphosphate (CTP), uridine triphosphate (UTP) and thymidine triphosphate (TTP) did not12. MDS show that ATP is extremely stably bound with the same orientation and interactions as ACP in the crystal structure (Fig. 4a and Supplementary Movie 1). ACP is therefore a reliable ATP analogue.
The ternary complex asBC contains two lipid substrates (MAG1, MAG2; Fig. 1a). MAG1 has been modelled into the electron density map with its headgroup deep in the protein positioned at the level of the membrane interface with its reactive 1-OH next to the γ-phosphate of ACP (Fig. 1c,f). MAG2 is in the putative lipid substrate-binding pocket, with its headgroup ∼4 Å from MAG1. Their acyl chains extend into the membrane along the hydrophobic surface of the protein. Since DAG, with two acyl chains, is the canonical lipid substrate of DgkA (ref. 2), finding a pair of MAGs as noted, implies they demark the lipid substrate-binding site.
The electron density for MAGs in the complex is variable and in parts, discontinuous (Supplementary Fig. 4a–d). However, in our studies of DgkA to date, we have crystal structures that include a total of 10 trimers with density in the active site for bound lipid that is variable (refs 12, 17 and this work). Mapping these onto a single active site makes a convincing case that lipids reside in the binding pocket (Supplementary Fig. 4e–g). Their variable definition likely reflects acyl chain flexibility and lipid movement during reaction.
The two other active sites in the complex lack nucleotide (Fig. 1b). asAB has two MAGs situated similar to those in asBC. Like asBC, asAB includes an almost complete SH that creates a well-defined active site. By contrast, the SH of asCA is not visible in density until Ser17A. Accordingly, this active site appears wide open (Fig. 1b). It contains just one, distant MAG.
Mutational studies have identified residues in DgkA that impact on catalysis (refs 9, 13 and this work). They include Thr8, Arg9, Ser17, Gly20, Glu28, Ala30, Glu34, Glu69, Asn72, Ser73, Glu76, Asp80, Gly83, Ser90, Lys94, Asp95, Gly97 and Ala100 (Fig. 2b). Convincingly, 14 out of the 18 are proximal (≤5 Å) to the nucleotide and lipid substrates in the ternary complex and all are exposed to solvent during the MDS (Fig. 3a–c, Supplementary Fig. 5). They demark the substrate binding and catalytic sites. The putative catalytic site resides on the protein at the membrane/cytosol interface where the reactive moieties of the two substrates, with disparate polarities, come together for reaction.
The active site includes glutamates and an aspartate predicted to play roles in substrate binding and catalysis (Fig. 3a,b). Concerns have been raised generally regarding possible X-ray damage to anionic residues18 and to irrelevant conformational substates trapped as a result of collecting diffraction data with an intense synchrotron microbeam at 100 K (refs 19, 20). To address these issues we have obtained a structure by serial femtosecond crystallography (SFX) with an X-ray free-electron laser (XFEL) at room temperature (RT) and ahead of radiation damage21,22,23 (Table 1). It suggests that damage and ‘frozen’ conformational substates were not major issues under current conditions and that the ternary complex structure reported here is reliable. Alternative conformers for side chains of three critical residues, Glu34, Glu69 and Glu76, were observed in the XFEL structure at RT that may be functionally relevant, as discussed (Fig. 5a,b,d,e).
Convincing kinetic and biochemical evidence supports a direct, in-line phosphoryl transfer mechanism for DgkA (ref. 2). This is in contrast to one that requires the formation of an enzyme-phosphate intermediate with subsequent phosphotransfer to the lipid substrate. The direct route displays a hallmark, trigonal bipyramidal phosphorus intermediate and a random kinetic pathway where one substrate does not exclude the binding of the other. Further, the γ-phosphate of ATP should be proximal to the 1-OH of the lipid substrate. This is what was observed in the ternary complex where the two entities are poised for reaction ∼4 Å apart (Fig. 3c). The separation is reminiscent of what has been interpreted for DgkA and for water-soluble kinases, where a tetraphosphate analogue of the bisubstrate (ATP-DAG in the case of DgkA) is a better inhibitor than the bisubstrate itself2. Presumably, the extra space accommodates both substrates, the reactive moieties of which are brought together for reaction by a small conformational change in the protein.
Glu69 is a conserved, essential residue in DgkA (refs 9, 13; Fig. 2b, Supplementary Table 1, Supplementary Fig. 1b). In the liganded asBC, its carboxyl is in hydrogen-bonding distance to the 1-OH of MAG1 (Fig. 3c). By analogy with other kinases24, we propose that Glu69 initiates catalysis by abstracting a proton from this primary hydroxyl. In this configuration, the proximal Glu34C (Fig. 5a, Supplementary Fig. 6, and Supplementary Fig. 7) is predicted to have a pKa of 7.53 and therefore will be protonated at neutral pH, acting as a hydrogen bond donor to Glu69C at rest. This is a stable configuration in the MDS. Due to the hydrophobic nature of the pocket, deprotonation of Glu34C will elevate the pKa of Glu69C making it a stronger base and a better general-base catalyst. We hypothesize, therefore, that deprotonation of Glu34C is the trigger for catalysis in a substrate-loaded enzyme. Interestingly, in the XFEL structure of the apo-enzyme there are two conformations for Glu34 and Glu69. One of each conformer has a matching partner in the cryo structure described above that can be isolated from the MDS by switching the protonation states of Glu34C and Glu69C. In the case of Glu69, the alternate conformation extends deeper into the membrane and has a predicted pKa value of 8.82. This is reflected in the MDS, where protonation of Glu69C induces a side-chain switch to this conformation and inversion of the hydrogen-bonding configuration with Glu34C. This is likely to be the side-chain rotamer after the proton has been removed from the primary hydroxyl of the lipid substrate. Alternatively, this may guide substrate lipid entering from the bilayer to the active site (Fig. 5d,e). With Glu34, the two conformers may also provide a switch that controls the pKa and basicity of Glu69. The lipid alkoxide formed on proton abstraction is in position to attack the γ-phosphate of ATP which leads to the formation of the pentavalent intermediate, stabilized by Asn72C and/or Arg9B (Figs 2a, 3b and 5c). Collapse of the intermediate severs the β−γ linkage, generating lyso-phosphatidic acid and ADP as products. Since both are negatively charged, product egress might be aided by electrostatic repulsion from anionic residues Glu69C and Glu76C in the active site, accompanied by metal-binding site rearrangement, and by cationic residues Arg9 and Lys12 in the SH proposed to draw the lipid out as the SH flexes away from the site (Fig. 4f). On release, the active site is reset for another round of catalysis, with Glu34 reprotonating from Glu69 (Supplementary Figs 6,7).
MDS show clearly that ADP is positionally unstable in the binding site (Fig. 4f, Supplementary Movie 1). DFT simulations on MDS-sampled configurations displaying intimate MAG1 contacts (similar to Fig. 3c) suggest that 1-OH proton abstraction by Glu69C is kinetically more accessible than phosphate cleavage (Supplementary Fig. 8, Methods section). In accord with the proposed pentavalent stabilization by Asn72C and/or Arg9B (Fig. 2a), the cleavage step is likely to be rate-limiting.
Two MAGs have been modelled in the liganded asBC. The 1-OH of MAG1 is proximal to the carboxyl of the putative catalytic Glu69C (Fig. 3c). Ser98C interacts with the 2-OH of MAG1 which, in the case of the canonical substrate DAG, would be in ester linkage to an acyl chain. The carbonyl oxygen at the ester linkage in MAG1 is within hydrogen-bonding distance of critically important Ser17B. Together, these interactions with highly conserved and/or critical residues fix the headgroup of the lipid substrate in position for proton abstraction by Glu69C and for reaction with the γ-phosphorus of ATP (Fig. 3c). The lipid acyl chains reside within or close to a three-walled hydrophobic pocket created by the transmembrane stretches of H1-3C (Supplementary Fig. 4e–g). The pocket appears to use the bulky and highly conserved Trp112C (Supplementary Table 1 and Supplementary Fig. 1b) with the plane of its indole ring oriented, by hydrogen bonding to Ser61C in the trimer core, to create a base for the pocket below which the chains do not extend (Supplementary Fig. 4f). Its location towards the bilayer mid-plane may contribute to defining lipid substrate chain-length preference.
Comparison with other kinases
In support of the proposed mechanistic model, we note the striking resemblance between critical residues in the active site of DgkA and their equivalents in cAMP-dependent protein kinase (PKA) for which a similar catalytic mechanism is well established24,25 (Fig. 2a). To begin with, the catalytic residue in both kinases is anionic, Glu69 in DgkA and Asp166 in PKA. While magnesium is a common ATP counter-ion in kinases, zinc can serve this role in DgkA (ref. 16). Both zinc ions in the ternary complex bind electrostatically with the γ-phosphate of ACP and, by electron withdrawing effects, render the phosphorus more susceptible to attack by the lipid nucleophile. The same kind of interaction is seen in PKA. Lys94C coordinates with the α-phosphate of ACP in a manner analogous to its counterpart, Lys72, in PKA. Lys94C is stabilized in position by a critical Asp80C, just like the Lys72-Glu91 pair in PKA. The essential Glu76C chelates the two zincs which, in turn, bind the triphosphate of ACP. The equivalent residue in PKA is Asp184. Parenthetically, a second conformation for the side chain of Glu76C is present in the XFEL apo-structure which is more removed from the metal ions; it may play a role in product release (Fig. 5b). Arg9 is functionally important and mutating it dramatically alters DgkA activity. While its side chain lacks full density in the DgkA complex, one of its possible conformers makes a convincing interaction with the α-phosphate of ACP, reminiscent of the role played by Lys168 in PKA. Asn72 is essential in DgkA (Fig. 2b and Supplementary Table 1). Its side-chain carbonyl is 4.1 Å from Zn2 while its amide nitrogen bridges the essential Glu69 and Glu76 (Fig. 5c). The equivalent residue in PKA is Asn171; it bridges Asp166 and Asp184 and its carbonyl is 2.1 Å from manganese (Mn1).
The similarity between the binding sites of DgkA and PKA extends to the adenosine end of the nucleotide. Thus, the aforementioned clamping triad on adenine in the CL of DgkA that includes Glu85-Tyr86-His87 is matched by an almost identical triad in PKA represented by Glu121-Tyr122-Val123 (Figs 2a and 6). At the same time, the two ribose hydroxyls are anchored by Asp95 in DgkA and by Glu127 in PKA. The resemblance between residues in and chemical architecture of the active sites of DgkA and PKA is remarkable given that the two kinases are evolutionarily unrelated and have essentially no primary through quaternary structure similarities.
With the ternary complex structure in hand, hypotheses regarding the role of specific residues in DgkA enzymatic activity were tested by systematic mutagenesis. Kinetic measurements were performed with the mutants reconstituted in the LCP. A total of 23 sites were mutated with the types screened dictated by the putative role for the particular residue. The results are summarized in Fig. 2b and Supplementary Table 1 along with data from separate mutational studies9,13. A few notable mutants will be discussed here, as follows. (i) Glu69 is the putative catalytic residue in DgkA (Figs 2a and 3c), in contrast to Asp which serves that function in serine protein kinases. Strikingly, Glu69 tolerated none of the mutations tested, one of which was Asp (pKa 3.8). This could be a spatial effect because the side chain of Asp is too short. It may also have to do with the fact that the 1-OH in glycerides like MAG and DAG have pKa values (13.6) higher than those of PKA substrates Ser/Thr (pKa 13.0). Glycerides therefore may require the carboxyl of Glu, with a pKa of 4.3, or higher enabled by nearby Glu34, for proton abstraction. (ii) The conserved Asp95 coordinates the hydroxyls of ribose in ACP, preserved throughout the MDS, and the carbonyl of Gly91 (Fig. 3a). Mutating it to Ala essentially abolished activity. However, Glu with its longer side chain did substitute but activity was reduced by 76%. By contrast, Asn had a minor effect which makes sense given that its side-chain amide can hydrogen bond with carbonyls and hydroxyls. (iii) Ala30 resides on H1 in the active site entrance at the membrane interface (Fig. 5f). Its methyl side chain was speculated to enable lipids with small headgroups to enter the site. Mutating it to the bulky leucine reduced activity by 93% consistent with a putative gatekeeping role. (iv) Gly83 in the CL was proposed to facilitate the helix-coil transition enabling adenine binding (Supplementary Fig. 3). Mutating it to Pro was expected to compromise such activity. Indeed, the Gly83Pro mutant was virtually dead enzymatically; MDS show dynamic instability of the CL (Supplementary Movie 2) and (v) finally, Asn72 plays a key role in catalysis. Its side-chain amide bridges Glu69 and Glu76 (Fig. 5c) both of which are essential. These H-bonds bridge the two essential residues throughout the MDS. The Asn72Ala mutant is catalytically inactive. For all intents and purposes, so too are the Asn72Gln and Asn72Asp mutants. These data show how important both the precise chemistry and the architecture of this part of the binding/active site are for catalysis. The structure-based, hypothesis-testing mutations and others in Fig. 2b and Supplementary Table 1 lend credence to the complex model and mechanism of kinase action.
DgkA is the tiniest of kinases. With just 121 residues and a trimeric constitution, three kinase catalytic sites have been fashioned (Fig. 1). Each acts at the membrane/cytosol interface. The rest of the protein creates binding pockets on either side that position the reactive ends of two large substrate molecules with dramatically different polarities in juxtaposition for reaction. The ternary structure explains in atomic detail how the nucleotide and lipid-binding sites interact with substrate molecules. The many, contact site-docking defines a specific orientation for the nucleotide that presumably is optimized for transphosphorylation. Particularly striking is the similarity between the binding site architecture of this bacterial DgkA and mammalian PKA (Figs 2a and 6), kinases that bear no resemblance at any other level of structure. Thus, these defined points of chemical constitution arrayed precisely in three-dimensional space have evolved independently achieving a similar end in entirely different protein contexts – a convincing case of convergent evolution.
DgkA’s small size shows that a functioning kinase can be built with very little protein mass. The ternary structure points to a minimum required for that purpose. Inspecting the complex suggests that a pair of helices, each 3-4 turns long, connected by a 7-residue loop (Supplementary Fig. 3) might be all that is needed to create an ATP-binding module. The ternary structure should serve as a template for rational protein and enzyme design, optimizable for solubility, stability, specificity and catalytic efficiency.
Kinetic studies suggest that DgkA functions with a moderate level of heteroallostery1. Thus, the binding of one substrate influences (in this case positively) that of its co-substrate. In a multimer like DgkA, it is possible for heteroallostery to come about through inter-subunit signalling. The fact that any given active site is a composite, with components from at least two subunits, suggests a way for the substrate-bound status of one site to be relayed to another; the SH is an obvious means for inter-subunit information transmission. In this way, the enzyme could present simultaneously three active sites in distinct states. We find some evidence for this in the ternary structure where only one of the three active sites is occupied by ACP. Further, two of the sites in the CL region, which clamps onto the nucleotide base, are profoundly different (Supplementary Fig. 3). Neither CL is involved in crystal contacts. Presumably therefore both are physiologically relevant. We propose that the three sites in DgkA are in different states at any given time during catalysis. However, it is possible to model a symmetrical DgkA trimer that is stable in MDS, indicating that the enzyme may adopt a symmetrical configuration. This does not imply that all three sites are catalytically active at the same time. Additional mechanistic and structure work is required to evaluate allosteric coupling within the enzyme.
As a trimer situated with half its bulk in the membrane and half in the cytosol, DgkA has features that make it a good biocatalyst. Its three active sites are arranged around the enzyme’s periphery (Fig. 1b) opening to the cytosol and the membrane for easy access and egress of substrates and products. This naturally raises the probability of productive encounters between substrates and binding sites, thus elevating the reaction rate compared to a hypothetical solitary active site. Conformational changes, where needed for turnover, would appear to be relatively minor involving small segments such as the CL for nucleotide and the SH for lipid and nucleotide binding. This should ensure efficient substrate loading and product release. The reduction in dimensionality, as a result of lipid substrate and enzyme confinement to a two-dimensional membrane, increases overall efficiency of delivery. The amphiphilic nature of the lipid and of the membrane in which it and the kinase reside, ensure the spontaneous and proper alignment of substrate in the lipid-binding site for reaction. These features of trimeric DgkA undoubtedly contribute to making it an efficient biocatalyst, described previously as an evolutionarily optimized integral membrane enzyme.
Molecular biology and protein production
All but two of the DgkA mutants were generated by PCR-based site-directed mutagenesis using the plasmid pTrcHisB-DgkA-WT (ref. 14) as the template. In the case of E34D and E34A, constructs with the desired mutation could not be produced after several rounds of mutagenesis trials. Instead, the corresponding genes were synthesized chemically (Genescript). All mutations were confirmed by DNA sequencing (MWG Biotech). Detailed purification procedures are described in ref. 14. Briefly, E. coli WH1061 cells carrying DgkA plasmids and grown in Luria-Bertani broth were induced at an optical density of 0.6 for 3 h at 37 °C with 1 mM IPTG. All subsequent steps were carried out at 4 °C unless otherwise specified. For crystallization, cells from 1 l of culture were lyased by sonication in buffer containing 0.2 mM TCEP, 0.3 M NaCl, 0.2 mg ml−1 lysozyme, 50 μg ml−1 DNAase, 10 μM BHT, 1 mM PMSF, 0.2 mM EDTA, 5 mM MgCl2 and 75 mM Tris/HCl pH 7.8. Empigen BB was added to the cell lysate at 3.3% (w/v) to solubilize DgkA for 1 h. Unsolublized material was removed by centrifugation at 9,000g for 10 min. The supernatant containing N-terminally His-tagged DgkA was allowed to bind to 4 ml of Ni-NTA resin for 1 h. The resin was packed in a gravity column, which was washed with 3% (w/v) Empigen BB, 10 mM imidazole in Buffer A (0.3 M NaCl, 0.2 mM TCEP, 40 mM HEPES pH 7.5) and 1.5% (w/v) Empigen BB, 40 mM imidazole in Buffer A. The detergent Empigen was then exchanged to n-decyl-β-D-maltopyranoside (DM) by washing the column with 12 column volumes of buffer containing 0.25% (w/v) DM, 50 mM LiCl, 0.2 mM TCEP, 20 mM HEPES pH 7.5. Protein was eluted with 0.25 M imidazole in buffer containing 0.5% (w/v) DM, 1 mM TECP, 50 mM LiCl and 10 mM HEPES pH 7.5. Pooled fractions were concentrated and run through a size-exclusion chromatography with a Superdex 200 16/600 column in buffer containing 0.25% (w/v) DM, 1 mM TCEP, 0.1 M NaCl and 10 mM Tris HCl pH 7.5. Fractions corresponding to the central peak were pooled. Protein was concentrated to 12 mg ml−1, flashed frozen in liquid nitrogen as 11 μl aliquots and stored at −80 °C until use. For functional assays, protein was purified from 0.1 l of cell culture, omitting the size-exclusion chromatography step. Size-exclusion chromatography had no effect on specific activity.
In meso measurements of WT and mutant DgkA kinase activity were carried out as follows15. DgkA was reconstituted into LCP by mixing the protein solution with a 1.5-fold volume of monoolein. Five microliters of LCP was dispensed into each well of a 96-well plate. The coupled enzyme assay reaction was initiated by adding 200 μl of Assay Mix (20 mM ATP, 0.1 mM EDTA, 0.1 mM EGTA, 55 mM magnesium acetate, 1 mM phosphoenolpyruvic acid, 0.2 mM dithiothreitol, 50 mM LiCl, 0.4 mM NADH, 20 U ml−1 of pyruvate kinase and lactate dehydrogenase, and 75 mM PIPES pH 6.9) pre-warmed to 30 °C. The decrease in A340, caused by the oxidation of NADH which is coupled to ATP–ADP conversion, was recorded every 6–10 s over a period of 1 h. For WT enzyme and fully functional constructs, the protein concentration used for reconstitution into the mesophase was 0.066 mg ml−1. For mutants with <∼70% of WT activity, protein concentration was adjusted to 0.1−5 mg ml−1 to increase measurement sensitivity.
In meso crystallization of the apo form of Δ4-DgkA for synchrotron radiation data collection was carried out using an in meso robot15. The 96-well glass sandwich crystallization plates were incubated at 4 °C for crystal growth15. The precipitant solution contained 7–9% (v/v) 2-methyl-2,4-pentanediol (MPD), 0.1 M NaCl, 0.1 M KNO3, 0.1 M Na3C6H5O7 (sodium citrate) pH 5.6 for 9.9 MAG, and 4—7% (v/v) MPD, 0.1 M NaCl, 0.06 M Mg(CH3COO)2 (magnesium acetate), 0.05 M Na3C6H5O7 for 7.9 MAG. Crystals were harvested and snap cooled in liquid nitrogen26.
To produce crystals of DgkA in complex with an ATP analogue, extensive screening was performed that involved exploring protein constructs, crystal forms, host MAGs, analogues, crystallization precipitants and temperature. Trials with Δ4-DgkA in 9.9 MAG with zinc-ACP at 4 °C eventually provided crystals and a structure at 2.70 Å resolution. Crystals were soaked directly in glass sandwich plates for 2 h at 4 °C using precipitant solution (7–10% (v/v) MPD, 0.1 M NaCl, 0.1 M KNO3, 0.1 M Na3C6H5O7 pH 5.6) supplemented with 60 mM Zn(CH3COO)2 and 10 mM ACP. Harvesting was performed, as noted above.
For measurements with the XFEL, crystallization was carried out at 20 °C in coupled micro-syringes using 7.9 MAG as host lipid27,28,29. The precipitant solution contained 0.2% (v/v) MPD, 0.1 M NaCl, 0.05 M Na3C6H5O7 pH 5.6. Microcrystals were identified by bright-field and polarized light microscopy, SONICC and tryptophan fluorescence at the Linac Coherent Light Source (LCLS). Crystal-laden mesophase was transferred to an LCP injector and extruded for data collection into an evacuated chamber at 20 °C, as described below.
Synchrotron data collection and processing
Synchrotron diffraction data were collected at beamline 23-ID-B, Advanced Photon Source (USA), I24, Diamond Light Source (UK) and PXII, Swiss Light Source (SLS, Switzerland) at 100 K. At the Advanced Photon Source, data were collected with a 1° oscillation and a 1-s exposure per frame, a collimated beam size of 10 μm, and a sample-to-detector distance of 350-500 mm, with a MAR 300 CCD detector using 1.033 Å X-rays. At the Diamond Light Source, data were collected with a 0.2° oscillation and a 0.2-s exposure per frame, a microfocus beam size of 10 μm and a sample-to-detector distance of 500–650 mm, with a Pilatus 6M detector using 0.978 Å wavelength X-rays. At the SLS, data were collected with a 0.1 oscillation and 0.1-s exposure per frame, a collimated beam size of 10 × 15 μm2 and a sample-to-detector distance of 450–600 mm, with a Pilatus 6M detector using 1.033 Å X-rays.
Synchrotron-derived diffraction data were reduced with xia2 (ref. 30) using XDS (ref. 31) and XSCALE (Table 1). Optimum data wedges were identified by data quality and isomorphous unit cell parameters. Complete data sets for Δ4-99MAG-ACP and Δ7-79MAG (Table 1) were obtained by merging data collected from 4 and 6 crystals, respectively. A single crystal was used for the anomalous data collected at the zinc edge (Zn-edge Δ4-99MAG-ACP in Table 1).
XFEL data collection and processing
XFEL data were collected using the CXI instrument32 at the LCLS at SLAC National Accelerator Laboratory27,33. The LCLS was operated at a wavelength of 1.302 Å (9.5 keV) delivering X-ray pulses of 50 fs pulse duration and with 8 × 1011 photons per pulse focused into a spot size of ∼1.5 μm × 1.5 μm2 using a pair of Kirkpatrick–Baez mirrors. Needle-shaped protein microcrystals ranging in length from 10 to 40 μm dispersed in the LCP were injected into the focus region at 0.17 μl min−1 using a continuously flowing LCP injector with a nozzle capillary diameter of 50 μm (ref. 27). Single-shot diffraction patterns of randomly oriented crystals were recorded at a rate of 7,200 patterns per minute (120 Hz) using the Cornell-SLAC hybrid Pixel Array Detector (CSPAD) detector34. The sample-to-detector distance of ∼122 mm corresponded to a maximum obtainable resolution of 2.0 Å at 1.302 Å wavelength. Data collection required 4.5 h of beamtime and used 42 μl mesophase corresponding to 220 μg protein.
A total of 1,987,632 frames were collected, of which 180,031 (9.1%) were identified as ‘hits’ having crystal diffraction by the software package Cheetah35, from which 140,440 (78.0%) could be indexed and integrated using CrystFEL (ref. 36). The location of individual sensors on the CSPAD detector was determined to better than one pixel error by comparison of predicted and observed Bragg peak locations, and was key to obtaining a high indexing rate and data quality. Reflection intensities from all indexed diffraction patterns were integrated without applying a per-pattern resolution cut-off and merged in Point Group mmm using CrystFEL to produce one set of reflection intensities for structure determination. XFEL data could be evaluated to 2.15 Å, with a CC* of 0.998 (0.30 in the highest resolution shell) and I/sigma of 19.0 (0.33 in the highest resolution shell). Selection of the highest resolution shell (2.18 Å) was based on CC* and on improvements in Rwork/Rfree values, as well as map quality on stepwise screening higher resolution limits (2.13, 2.15, 2.18, 2.2 and 2.4 Å) during refinement37.
Structure solution, model building and refinement
Structures were solved by molecular replacement (MR) using published models (PDB ID: 3ZE3 and 3ZE4) with Phaser38. Coot39 and Phenix40 were used for manual building and refinement, respectively. Ligands were built based on feature enhanced maps41 and composite omit 2Fo-Fc maps. Lang et al.42 reported that the noise level in 2Fo-Fc maps is generally over estimated. Accordingly, the 2Fo-Fc map contoured at 0.7 σ, together with the strong electron density in the chain region of other DgkA structures (Supplementary Fig. 4), informed building the acyl chain of MAG1 in the asBC active site. The position of the two zinc ions were fixed during refinement based on an anomalous difference map (Fig. 1e) generated from X-ray diffraction data collected at the zinc edge (1.28238 Å, Table 1). The feature enhanced map (FEM)41 of the Zn-ACP moiety was calculated as follows. MR was performed with a DgkA trimer crystallized in the absence of nucleotide and an FEM was calculated directly from the MR solution using Phenix without adding nucleotide to the model. For the MAG1, the FEM was calculated as for the Zn-ACP but with MAG1 in place. Figures were prepared using PyMol.
Molecular dynamics simulations
All MDS were performed using GROMACS v5.0 (ref. 43). Initial Coarse Grained (CG) MD simulations using the Martini 2.2 force field were run for 1 μs to permit the assembly and equilibration of a dipalmitoylphosphatidylglycerol (DPPG): dipalmitoylphosphatidylethanolamine (DPPE; 1:3 mole ratio) bilayer around DgkA (ref. 44). The end-snapshot of the CG simulations were then converted to atomic detail with the crystal structure aligned with the CG protein within the assembled lipid bilayer45. The systems were then equilibrated for 1 ns with the protein restrained before 100 ns of unrestrained atomistic MD using the Gromos53a6 force field46. In almost all cases, ATP, Zn2+ and MAG were included. In one instance, GTP was included instead of ATP. In a second case, ADP and lyso-phosphatidic acid were included in place of ATP and MAG. Parameters for catalytic intermediates were also designed, with the associated coordinates simulated in the complex. Systems were neutralized with a 150-mM concentration of NaCl. In silico mutagenesis was performed using PyMol.
Density functional theory
Modelling chemical reactions is not possible with (classical) MDS. Accordingly, using ab initio-based DFT molecular-simulation techniques to probe putative reaction paths and energetics is of relevance and help to enzyme reaction mechanism studies. Gaussian 09 software B3LYP/6-31G(d,p) simulations were performed on MDS configurations like Fig. 3c, featuring intimate MAG1 contacts; other configurations were less energetically plausible. MM (AMBER), ONIOM-QM/MM (ref. 47) and DFT geometry-optimization led to retaining zinc atoms and residues within ∼7 Å (244 atoms) and ∼8 Å (365 atoms) of MAG1, for MAG1’s reliable energetic and geometric interactions.
Examining carefully MDS-sampled, ‘cut-down’ configurations of the ternary complex’s active site similar to Fig. 3c, the energetics of possible interactions of 1-OH with neighbouring protein residues were studied. Both geometry optimization and systematic movement of the lipid substrate’s 1-OH proton towards nearby residues were used to examine the change in the system's energy along this proton abstraction path. In DFT, albeit approximate, the electron probability density around nuclei is determined, so geometry optimization can ‘relax’ and move the nuclear coordinates to lower the system’s energy to a (local or global) minimum. Relaxation of particular configurations could include 1-OH proton transfer, or rearrangement of bonds, or the formation of a (near-) covalent bond between an 1-O oxyanion (or even 1-OH with proton intact) and the γ-phosphorus atom to form a pentavalent intermediate structure (Supplementary Fig. 6). A key point regarding these possible events is their energetic (and kinetic) ‘accessibility’, especially in relation to background thermal energy ∼RT. At room temperature (RT) is around 0.6 kcal mol−1. Accordingly, such reaction events accessible for routine observation during geometry optimization would typically have energy barriers of ∼2–3 kcal mol−1, or less. Indeed, the connection between reaction-energy barriers and approximate rates is well-established in chemical kinetics. On this basis, we found that the only likely interaction with protein residues for reaction of 1-OH was with Glu69, featuring a prominent hydrogen bond with the proton in 1-OH pointing directly to Glu69. In some cases, geometry optimization entailed the direct transfer of the proton to Glu69, suggesting an energy barrier of ∼2–3 kcal mol−1, or less. The relative potential-energy profile for this is shown in Supplementary Fig. 8b, where the ‘kink’ in slope denotes the rupture of the O–H covalent bond prior to formation of the bond with Glu69. Because movement along this direct path (cf. Supplementary Fig. 8a) does not necessarily follow a minimum-energy path across the potential-energy landscape (akin to taking an ‘as-the-crow-flies’ route through a valley, rather than following a slightly meandering river), the ∼5 kcal mol−1 barrier is an overestimate, and direct transfer in structure relaxation suggests the actual barrier is lower (see above). The sharply ‘downhill’ energetic nature of proton transfer indicates an approach towards spontaneity for this event. This transfer is facilitated greatly by the prominent hydrogen bond’s strong electrostatic interaction, especially given the high charge-to-mass ratio of the proton.
Optimization of the alkoxide form led to the formation of a somewhat strained, imperfect covalent bond for the resultant (1-O) oxyanion (sans proton) with the γ-phosphorus atom, not unusual for a pentavalent intermediate, suggesting reasonable kinetic accessibility with a ∼2–3 kcal mol−1 barrier. However, further structure relaxation did not suggest any rupture (or meaningful stretch/strain) of the bridging γ-P–O bond. Extending systematically this covalent bond until breakage, the relative potential-energy profile (Supplementary Fig. 8b) suggests a reaction-energy barrier of ∼15 kcal mol−1. Unlike the hydrogen bond in proton transfer, there is no appreciable local electrostatic interaction in this bond. The much larger mass of P and O atoms and inertia of the MAG1 and to-be-formed ADP moieties compounds this, altering the character of this potential-energy profile. With a large positive barrier to be crossed, it is much less kinetically favourable. Here, the substantial positive-energy ‘hill’ shows clearly the unfavourable nature of extending the bond from a local minimum in the immediate vicinity of the ‘reactant’ state, hindered by less electrostatic interaction, until rupture beyond 0.5–0.6 Å. This is somewhat consistent with previous computational estimates of 26.7 kcal mol−1 (based on potential-energy differences), albeit for cleavage of ATP (only) in explicit water, and not in the current protein milieu48. Such ‘as-the-crow-flies’ overestimates of energy barriers vis-à-vis relatively (but not completely) ‘straight’ paths (akin to those shown in Supplementary Fig. 8a and traversed in b) is around double. This would suggest a γ-P–O cleavage energy barrier of ∼8–10 kcal mol−1. This substantially larger value compared with proton abstraction indicates that phosphate cleavage is rate-limiting. This is consistent with the proposed stabilization by Asn72 and/or Arg9 of the pentavalent intermediate (Fig. 2a), and MDS evidence pointing to Arg9-mediated stabilization.
Accession codes: Atomic coordinates and structure factors for Δ4-99MAG-ACP, Δ4-99MAG, Δ7-79MAG-FEL and Δ7-79MAG are deposited in the Protein Data Bank under accession codes 4UXX, 4UXW, 4UYO and 4UXZ, respectively.
How to cite this article: Li, D. et al. Ternary structure reveals mechanism of a membrane diacylglycerol kinase. Nat. Commun. 6:10140 doi: 10.1038/ncomms10140 (2015).
Van Horn, W. D. & Sanders, C. R. Prokaryotic diacylglycerol kinase and undecaprenol kinase. Annu. Rev. Biophys. 41, 81–101 (2012).
Badola, P. & Sanders, C. R. Escherichia coli diacylglycerol kinase is an evolutionarily optimized membrane enzyme and catalyzes direct phosphoryl transfer. J. Biol. Chem. 272, 24176–24182 (1997).
Lau, F. W., Chen, X. & Bowie, J. U. Active sites of diacylglycerol kinase from Escherichia coli are shared between subunits. Biochemistry 38, 5521–5527 (1999).
Mi, D., Kim, H. J., Hadziselimovic, A. & Sanders, C. R. Irreversible misfolding of diacylglycerol kinase is independent of aggregation and occurs prior to trimerization and membrane association. Biochemistry 45, 10072–10084 (2006).
Sanders, C. R. et al. Escherichia coli diacylglycerol kinase is an alpha-helical polytopic membrane protein and can spontaneously insert into preformed lipid vesicles. Biochemistry 35, 8610–8618 (1996).
Li, D. & Caffrey, M. Renaturing membrane proteins in the lipid cubic phase, a nanoporous membrane mimetic. Sci. Rep. 4, 5806 (2014).
Nagy, J. K., Lau, F. W., Bowie, J. U. & Sanders, C. R. Mapping the oligomeric interface of diacylglycerol kinase by engineered thiol cross-linking: homologous sites in the transmembrane domain. Biochemistry 39, 4154–4164 (2000).
Smith, R. L., O'Toole, J. F., Maguire, M. E. & Sanders, C. R. Membrane topology of Escherichia coli diacylglycerol kinase. J. Bacteriol. 176, 5459–5465 (1994).
Wen, J., Chen, X. & Bowie, J. U. Exploring the allowed sequence space of a membrane protein. Nat. Struct. Biol. 3, 141–148 (1996).
Zhou, Y. & Bowie, J. U. Building a thermostable membrane protein. J. Biol. Chem. 275, 6975–6979 (2000).
Lau, F. W., Nauli, S., Zhou, Y. & Bowie, J. U. Changing single side-chains can greatly enhance the resistance of a membrane protein to irreversible inactivation. J. Mol. Biol. 290, 559–564 (1999).
Li, D. et al. Crystal structure of the integral membrane diacylglycerol kinase. Nature 497, 521–524 (2013).
Van Horn, W. D. et al. Solution nuclear magnetic resonance structure of membrane-integral diacylglycerol kinase. Science 324, 1726–1729 (2009).
Li, D., Shah, S. T. & Caffrey, M. Host lipid and temperature as important screening variables for crystallizing integral membrane proteins in lipidic mesophases. trials with diacylglycerol kinase. Cryst. Growth Des. 13, 2846–2857 (2013).
Li, D. & Caffrey, M. Lipid cubic phase as a membrane mimetic for integral membrane protein enzymes. Proc. Natl Acad. Sci. USA 108, 8639–8644 (2011).
Walsh, J. P. & Bell, R. M. sn-1,2-Diacylglycerol kinase of Escherichia coli. Mixed micellar analysis of the phospholipid cofactor requirement and divalent cation dependence. J. Biol. Chem. 261, 6239–6247 (1986).
Boland, C. et al. Cell-free expression and in meso crystallisation of an integral membrane kinase for structure determination. Cell. Mol. Life Sci. 71, 4835–4910 (2014).
Burmeister, W. P. Structural changes in a cryo-cooled protein crystal owing to radiation damage. Acta Crystallogr. D Biol. Crystallogr. 56, 328–341 (2000).
Fraser, J. S. et al. Accessing protein conformational ensembles using room-temperature X-ray crystallography. Proc. Natl Acad. Sci. USA 108, 16247–16252 (2011).
Halle, B. Biomolecular cryocrystallography: structural changes during flash-cooling. Proc. Natl Acad. Sci. USA 101, 4793–4798 (2004).
Chapman, H. N. et al. Femtosecond X-ray protein nanocrystallography. Nature 470, 73–77 (2011).
Spence, J. C., Weierstall, U. & Chapman, H. N. X-ray lasers for structural and dynamic biology. Rep. Prog. Phys. 75, 102601 (2012).
Chapman, H. N., Caleman, C. & Timneanu, N. Diffraction before destruction. Philos. Trans. R. Soc. Lond. B Biol. Sci. 369, 20130313 (2014).
Endicott, J. A., Noble, M. E. & Johnson, L. N. The structural basis for control of eukaryotic protein kinases. Annu. Rev. Biochem. 81, 587–613 (2012).
Zheng, J. et al. 2.2 A refined crystal structure of the catalytic subunit of cAMP-dependent protein kinase complexed with MnATP and a peptide inhibitor. Acta Crystallogr. D Biol. Crystallogr. 49, 362–365 (1993).
Li, D., Boland, C., Aragao, D., Walsh, K. & Caffrey, M. Harvesting and cryo-cooling crystals of membrane proteins grown in lipidic mesophases for structure determination by macromolecular crystallography. J. Vis. Exp. 67, e4001 (2012).
Weierstall, U. et al. Lipidic cubic phase injector facilitates membrane protein serial femtosecond crystallography. Nat. Commun. 5, 3309 (2014).
Caffrey, M., Li, D., Howe, N. & Shah, S. T. 'Hit and run' serial femtosecond crystallography of a membrane kinase in the lipid cubic phase. Philos. Trans. R. Soc. Lond. B Biol. Sci. 369, 20130621 (2014).
Liu, W., Ishchenko, A. & Cherezov, V. Preparation of microcrystals in lipidic cubic phase for serial femtosecond crystallography. Nat. Protoc. 9, 2123–2134 (2014).
Winter, G., Lobley, C. M. & Prince, S. M. Decision making in xia2. Acta Crystallogr. D Biol. Crystallogr. 69, 1260–1273 (2013).
Kabsch, W. Xds. Acta Crystallogr. D Biol. Crystallogr. 66, 125–132 (2010).
Boutet, S. & Williams, G. J. The Coherent X-ray Imaging (CXI) instrument at the Linac Coherent Light Source (LCLS). New J. Phys. 12, 035024 (2010).
Liu, W. et al. Serial femtosecond crystallography of G protein-coupled receptors. Science 342, 1521–1524 (2013).
Herrmann, S. et al. CSPAD-140k: a versatile detector for LCLS experiments. Nucl. Instr. Meth. Phys. Res 718, 550–553 (2013).
Barty, A. et al. Cheetah: software for high-throughput reduction and analysis of serial femtosecond X-ray diffraction data. J. Appl. Crystallogr. 47, 1118–1131 (2014).
White, T. A. et al. CrystFEL: a software suite for snapshot serial crystallography. J. Appl. Crystallogr. 45, 335–341 (2012).
Karplus, P. A. & Diederichs, K. Linking crystallographic model and data quality. Science 336, 1030–1033 (2012).
McCoy, A. J. et al. Phaser crystallographic software. J. Appl. Crystallogr. 40, 658–674 (2007).
Emsley, P. & Cowtan, K. Coot: model-building tools for molecular graphics. Acta Crystallogr. D Biol. Crystallogr. 60, 2126–2132 (2004).
Adams, P. D. et al. PHENIX: a comprehensive Python-based system for macromolecular structure solution. Acta Crystallogr. D Biol. Crystallogr. 66, 213–221 (2010).
Afonine, P. V. et al. FEM: feature-enhanced map. Acta Crystallogr. D Biol. Crystallogr. 71, 646–666 (2015).
Lang, P. T., Holton, J. M., Fraser, J. S. & Alber, T. Protein structural ensembles are revealed by redefining X-ray electron density noise. Proc. Natl Acad. Sci. USA 111, 237–242 (2014).
Pronk, S. et al. GROMACS 4.5: a high-throughput and highly parallel open source molecular simulation toolkit. Bioinformatics 29, 845–854 (2013).
Stansfeld, P. J., Jefferys, E. E. & Sansom, M. S. Multiscale simulations reveal conserved patterns of lipid interactions with aquaporins. Structure 21, 810–819 (2013).
Stansfeld, P. J. & Sansom, M. S. P. From coarse grained to atomistic: a serial multiscale approach to membrane protein simulations. J. Chem. Theory Comput. 7, 1157–1166 (2011).
Oostenbrink, C., Villa, A., Mark, A. E. & van Gunsteren, W. F. A biomolecular force field based on the free enthalpy of hydration and solvation: the GROMOS force-field parameter sets 53A5 and 53A6. J. Comput. Chem. 25, 1656–1676 (2004).
Vreven, T., Morokuma, K., Farkas, O., Schlegel, H. B. & Frisch, M. J. Geometry optimization with QM/MM, ONIOM, and other combined methods. I. Microiterations and constraints. J. Comput. Chem. 24, 760–769 (2003).
Harrison, C. B. & Schulten, K. Quantum and classical dynamics simulations of ATP hydrolysis in solution. J. Chem. Theory Comput. 8, 2328–2335 (2012).
The work was supported by Science Foundation Ireland grant 12/IA/1255 (M.C.) and 07/SRC/B1160 (J.M.D. MacElroy), the National Institutes of Health Common Fund in Structural Biology grants P50 GM073210 (M.C.), R01 GM095583 (P.F.) and R01 GM108635 (V.C.); National Institute of General Medical Sciences GM75915 (M.C.) and U54 GM094599 (P.F.); and NSF Science and Technology Center award 1231306 (J.C.H.Spence). P.J.S. is supported by BBSRC grant BB/I019855/1. Work in MSPS’s lab is supported by the Wellcome Trust. C.G. kindly thanks the PIER Helmholtz Graduate School and the Helmholtz Association for financial support. All MD and most DFT simulations were performed using Irish Centre for High-End Computing (ICHEC) facilities, and we thank M. Peters for assistance. We thank C. R. Sanders for providing E. coli strain WH1061. The assistance and support of beamline scientists at the Advanced Photon Source (23-ID), Diamond Light Source (I24), Swiss Light Source (PXII) and LCLS, a National User Facility operated by Stanford University on behalf of the U.S. Department of Energy, Office of Basic Energy Sciences. We thank V. Pye for help with diffraction data collection and preliminary analysis, S. Knapp for advice on kinases, J. Holton for advice on data analysis, and S. Shah for lipid synthesis. J. Spence, E. Xu and R. Stevens are thanked for their encouragement and support.
The authors declare no competing financial interests.
Supplementary Figures 1-8, Supplementary Table 1 and Supplementary References. (PDF 1943 kb)
DgkA MD Simulations. a, DgkA trimer in a lipid bilayer. ATP and MAG1 shown as yellow spheres. Zinc ions shown as grey spheres. Phosphate lipid head group atoms shown as orange spheres. b, Focus on the ATP binding site. ATP and residues E28, N72, E76, E85, H87, K94 and D95 shown as sticks. The stability of the dynamics highlights the high fidelity of the crystal structure coordinates. c, Simulations with ADP and LPA, shown as sticks. The Zn1 ion moves to bridge the α- and β-phosphates of ADP. This slightly repositions the ADP molecule, so that K94 interacts with both α- and β-phosphates. The relocation removes the K94 hydrogen bond with N7 and thus the adenine ring is more likely to move, breaking the hydrogen bonds with E85 and H87. Once free, the enhanced adenine dynamics ruptures the hydrogen bonds with D95, leaving only interactions between Zn1 and K94 and the two remaining phosphates. Zn2 bridges the β-phosphate of ADP and the phosphate of LPA in this state. (MOV 25643 kb)
DgkA Mutant MD Simulations. In each case, the mutated residue is identifiable by a black sphere. a, E28A. In the simulations, the zinc-ATP complex moves towards the cytoplasm, away from the membrane and the MAG1 head group. Loss of the E28 side chain is likely to affect the binding of Zn2 in the absence of ATP. b, E76A. To compensate for the loss of E76, the zinc-ATP complex moves towards the membrane, so that E69 can fulfil the role of E76 in coordinating the two zinc ions. c, G83P. The proline mutation (spheres) appears to destabilise the CL, breaking the hydrogen bonds between the adenine ring and E85 and H87. d, K94A. This mutation rapidly destabilises both the adenine ring and α-phosphate of ATP due to loss of hydrogen bonds. As a result, the head group of ATP flips out of the binding site. (MOV 20236 kb)
About this article
Cite this article
Li, D., Stansfeld, P., Sansom, M. et al. Ternary structure reveals mechanism of a membrane diacylglycerol kinase. Nat Commun 6, 10140 (2015). https://doi.org/10.1038/ncomms10140
Communications Biology (2021)
Scientific Reports (2019)
Crystal structure of undecaprenyl-pyrophosphate phosphatase and its role in peptidoglycan biosynthesis
Nature Communications (2018)
Lipidic cubic phase injector is a viable crystal delivery system for time-resolved serial crystallography
Nature Communications (2016)