The gastric proton pump H+,K+-ATPase acidifies the gastric lumen, and thus its inhibitors, including the imidazo[1,2-a]pyridine class of K+-competitive acid blockers (P-CABs), have potential application as acid-suppressing drugs. We determined the electron crystallographic structure of H+,K+-ATPase at 6.5 Å resolution in the E2P state with bound BYK99, a potent P-CAB with a restricted ring structure. The BYK99 bound structure has an almost identical profile to that of a previously determined structure with bound SCH28080, the original P-CAB prototype, but is significantly different from the previously reported P-CAB-free form, illustrating a common conformational change is required for P-CAB binding. The shared conformational changes include a distinct movement of transmembrane helix 2 (M2), from its position in the previously reported P-CAB-free form, to a location proximal to the P-CAB binding site in the present BYK99-bound structure. Site-specific mutagenesis within M2 revealed that D137 and N138, which face the P-CAB binding site in our model, significantly affect the inhibition constant (Ki) of P-CABs. We also found that A335 is likely to be near the bridging nitrogen at the restricted ring structure of the BYK99 inhibitor. These provide clues to elucidate the binding site parameters and mechanism of P-CAB inhibition of gastric acid secretion.
The H+,K+-ATPase enzyme utilises ATP hydrolysis to drive electroneutral exchange of cytoplasmic protons for luminal K+, thus acidifying the gastric juice1, 2. Proton pump inhibitors (PPIs), such as omeprazole, are currently administered to suppress acid secretion in the treatment of acid-related diseases such as gastric ulcer or gastroesophageal reflux3. Acid suppression, in combination with antibiotics, is required for eradication of the gastric bacterium Helicobacter pylori. PPIs are weak bases that become protonated and accumulate in the acidic gastric lumen where they are converted to active sulfonamides and inhibit acid secretion by reacting covalently with cysteines accessible on the luminal side of H+,K+-ATPase (Fig. S1A)4. This mechanism results in a relatively slow onset of acid inhibition. The short dwell-times of PPIs in the blood and their instability under acidic conditions also negatively affect their efficacy as acid-suppressing drugs. Another class of H+,K+-ATPase drugs, K+-competitive acid blockers (P-CABs), are under development and some are now available for clinical use (Fig. S1B). The rapid and long-lasting acid suppression by P-CABs is expected to provide more immediate and efficient therapy for acid-related disease5. SCH28080 contains a imidazo[1,2-a]pyridine framework shared by a large subclass of P-CABs that competitively inhibit binding of the stimulating counterion, K+ (Fig. 1)6. Clinical application of SCH28080, however, is infeasible due to its toxicity. BYK99 has a chemical structure similar to that of SCH28080, except that the orientation of the imidazo[1,2-a]pyridine ring and the phenyl group is restricted by the addition of a diol bridge (Fig. 1), which results in BYK99 having more than 20-fold higher affinity than SCH280807. Based on the mutually antagonistic binding of omeprazole and SCH280808, as well as SCH28080 and BYK999, we investigated the possible binding site overlap of these inhibitors. A detailed understanding of the SCH28080 and BYK99 binding sites could facilitate the rational design of improved acid-suppressing drugs.
We previously reported a cryo-electron microscopy (cryo-EM) structure for H+,K+-ATPase with bound SCH28080 at 7 Å resolution and identified its binding location in a cavity facing the gastric lumen10. We demonstrated that the SCH28080 binding site formed as a consequence of the conformational rearrangement of the enzyme structure that includes transmembrane helices M1 to M4 and the A domain with its connecting linker to the M2 helix11, 12. The EM density corresponding to the bound SCH28080 was only partially visible, however, and neither its orientation nor its detailed interactions with the surrounding amino acid residues could be determined explicitly. The present study demonstrates a different P-CAB, BYK99, binds in the same general cavity and generates a similar global binding conformation.
Results and Discussion
Analysis of the BYK99-bound structure
We employed electron crystallography of two-dimensional crystals to determine the structure of H+,K+-ATPase at 6.5 Å resolution. BYK99 and beryllium fluoride were added to generate the E2P state with bound BYK99 [(BYK)E2BeF] (Fig. 2, Table S1). The quality of the density map of the BYK99-bound form analysed at 6.5 Å resolution was significantly improved over that of the 7 Å structure with bound SCH28080 [(SCH)E2BeF]10. The density assigned to bound BKY99 was observed in the luminal opening (Fig. 2D, Fig. S2), in a position that well overlapped the previously identified SCH28080 binding site (Fig. S3BC). This finding is consistent with the previously reported mutually exclusive binding of the two inhibitors, SCH28080 and BYK999. The molecular envelope of the cytoplasmic domains were well defined (Fig. 2B) and the transmembrane (TM) helices were observed as separate cylindrical densities in the (BYK)E2BeF structure (Fig. 2C, Fig. S2). These features are comparable to the other EM structures of H+,K+-ATPase so far determined. (BYK)E2BeF exhibited an almost identical molecular conformation as (SCH)E2BeF (Fig. S3A,D). Namely, the arrangement of the TM helices as well as the relative orientation of the cytoplasmic domains, and also the α-helical structure of the linker region connecting the A domain and M2 in the BYK99-bound form, were very similar to those of bound SCH2808010. When compared with the E2P transition state E2AlF11, where the luminal vestibule is closed, the (BYK)E2BeF (Fig. 2E) conformation exhibited an open vestibule where the M3M4 helix bundle bends outwardly at the luminal membrane interface and the M1-M2 helix bundle is near the bound BYK99. This conformation with an open vestibule is suggested to provide luminal access for the exchange of protons for K+ during the transport cycle13, and is similar to the ouabain-bound E2P state for Na+,K+-ATPase13 and the BeF-bound E2P “ground state” for SERCA14. The latter has also been proposed as the conformation associated with Ca2+ release to the lumen. These similarities among related P2-type ATPases suggest that the open E2P conformation is required for P-CABs to gain access to the binding cavity. Binding within the cavity would displace ordered water from both the cavity and the P-CAB, thus favouring the stability of the bound state. The present cryo-EM results provide direct evidence for a mechanism underlying the competitive inhibition by P-CABs, in which inhibitor binding blocks access of K+ from the lumen to its transport site and, conversely, binding of K+ at the transport site gives ion occlusion and closure of luminal access to the inhibitor binding cavity.
Evaluation of the proximity of M2 and the P-CAB binding site by site-directed mutagenesis
Our structural analyses revealed overlapping binding positions for SCH28080 and BYK99 (Fig. S3) and a common molecular conformation for H+,K+-ATPase. The M2 helix was in close proximity to the P-CAB binding site in the P-CAB bound state, but largely displaced from this position in the absence of the inhibitor (Fig. 2E). Mutagenesis of M2 was therefore investigated to identify the side-chains important for high-affinity binding. The wild-type (WT) or mutant α-subunit of H+,K+-ATPase was co-expressed with the β-subunit in HEK293S GnT1− cells15, and the ATPase activity in permeabilised membrane fractions was measured. In addition to SCH28080 and BYK99, we synthesised their derivatives: SCH-Me−, SCH-CN− for SCH28080, and BYK73 for BYK99 (Fig. 1, Fig. S6), and characterised their affinities and modes of inhibition. Most of the mutants retained sufficient activity for characterisation of the K+-competitive kinetics of inhibition by SCH28080 (Table S2 and Fig. S4). Affinity (inhibition constant, Ki) was calculated as described in the Materials and Methods16. Table 1 summarises the Ki of the compounds found for enzymes with a mutated M2. A striking finding was that mutations at amino acids D137 and N138 showed large changes in affinity for all compounds evaluated. The effects were similar in magnitude to some of those reported for mutations of amino acids likely to interact with bound SCH2808017,18,19,20,21,22,23, including A335C/C813A (Ki > 40,000 nM, ref. 20), L809F (Ki = 6150 nM)20, and Y799A (~100-fold low apparent affinity [IC50])21. Surprisingly, the N138A mutant exhibited more than 20-fold higher affinity for SCH28080 than for the WT enzyme. Similar increased affinity was observed for SCH-Me− and BYK99, but not for SCH-CN−, suggesting that the smaller side-chain of the mutant relaxes the length or conformational constraints for inhibitor binding. In contrast, hydrophobic mutations N138L and N138I had differing effects on inhibitor affinity (Table 1), indicating that the hydrophobic surface in this part of the binding site is important. In marked contrast to the D137 and N138 mutants, mutations of other amino acids in the M2 helix (D136, L139, and Y140) exhibited affinities almost comparable to the WT enzyme for all evaluated compounds, clearly indicating that these amino acids are not directly involved in the binding of SCH28080 or other tested chemicals. Also, mutations of the M1 helix did not have a significant effect on P-CAB affinity (Table 2), indicating that M1 does not directly contribute to P-CAB binding. Mutagenesis of the M2 helix showed that only mutations at D137 and N138 affected SCH28080 affinity (Table 1). This part of M2 is in close proximity to the inhibitor after rearrangement of the TM helices to give the P-CAB bound structures (Fig. 2E); hence, the inhibitor binding site is bounded by M2 on one side, and by M4, M5, and M6 helices on the other.
Effect of negatively-charged residue at the M2 helix
SCH28080 and other P-CABs behave as weak bases with the pKa of imidazo[1,2-a]pyridine (pKa = 5.6) giving only approximately 2.5% protonation at the pH of our ATPase assays (pH 7.0). It was previously proposed, however, that protonated SCH28080 binds with higher affinity. D137 is the only acidic amino acid in the M2 helix near the binding site in our model, and its accessibility to the solvent in the absence of the inhibitor is expected to give it a negative charge. This led us to evaluate a possible charge effect at the position of D137 (Table 3). As shown in Table 3, a D137N mutant displayed more than 60-fold lower affinity for both SCH28080 and BYK99 (Ki > 10,000 nM and 450 nM, respectively) than WT. The magnitude of these differences suggests that strong charge-pairing between D137 and the imidazo[1,2-a]pyridine ring is important for the binding. Although the Ki value of the charge-conserved mutant D137E could not be readily determined from global fitting due to its unusual kinetic parameters (see Materials and Methods), its affinity (Ki’) determined from a Km/Vmax plot indicated a smaller effect on the SCH28080 and BYK99 binding affinity (Ki’[SCH28080]D137E = 170 nM and Ki [BYK99]D137E = 57 nM, respectively). Introduction of a negative charge at the neighbouring N138 (N138D) had no significant effect on P-CAB affinity. Although the charge-swapped double mutant (D137N/N138D) exhibited reduced affinities for the P-CABs compared with the WT, its effect was much smaller than that of the single D137N mutant. This observation indicates that introducing a negative charge at the position close to D137 can partially, but not completely, compensate for the charge-neutralisation in the D137N mutant, and thus the correct orientation of the charged side-chain is also important for inhibitor binding. Therefore, the negatively charged side-chain of D137 in the M2 helix is in proximity to the imidazo[1,2-a]pyridine of SCH28080 and other related P-CABs, perhaps directly stabilising the positively-charged inhibitor where tight binding in the site would exclude water and prevent access to the bulk solvent. Under physiological conditions where the luminal pH is low, exclusion of water in the bound state could also prevent protonation of D137 to preserve the charge interaction. These data however could not exclude the possibility that the negatively-charged D137 indirectly affects inhibitor affinity. For example, D137 may be important for formation of the binding site itself by interacting with neighbouring side-chains.
Mutants of the M3-M6 helices
Previous extensive mutagenesis studies suggested some key amino acids likely to interact directly with SCH2808017,18,19,20,21,22,23. To confirm that our measurements were consistent with these results, and to confirm whether low-affinity SCH28080 derivatives (SCH-Me−, SCH-CN−, and BYK73) show binding behaviour similar to the parent compound, we selected various previously reported mutations and assayed them in the presence of these compounds (Table 3). C813 (M6) forms a covalent S-S bond with omeprazole, and omeprazole binding is antagonistic with respect to SCH280803. We therefore tested the double mutant A335C (M4)/C813A (M6), which has almost no affinity for SCH2808020. Y799A (M5) has a 100-fold reduced apparent affinity (IC50) for SCH28080, while the Y799F mutant has negligible effects on SCH28080 affinity, suggesting the importance of the phenyl group on this tyrosine residue21. Mutation of L809 for phenylalanine (M5M6 loop) led to a more than 90-fold reduced affinity. These mutations all showed similar results when reproduced in the present study, and the derivatives shown in Fig. 1 and Table 3 exhibited similar tendencies in their affinity changes. In addition, all of the compounds evaluated in this study showed competitive inhibition with respect to the K+ concentration regardless of their different affinities (Fig. S5). Therefore, we concluded that, despite the significantly lower affinity of SCH-Me−, SCH-CN−, and BYK73 compared with the original compounds, these derivatives apparently share a similar binding mode.
A remarkable difference was observed between the WT and A335G mutant with respect to their affinities for BYK73 (Table 3), a compound in which the bridging nitrogen is methylated (Fig. 1). Due to this methyl group modification, the WT enzyme has a 1000-fold lower affinity for BYK73 compared with BYK99 (Ki[BYK73]WT = 4.9 μM and Ki[BYK99]WT = 5.8 nM). Substitution of A335 with the smaller glycine partially compensates for the effect of the methyl group with more than 60-fold increased affinity for BYK73 (Ki[BYK73]A335G = 78 nM). This contrasts with the 5-fold increase for BYK99 (Ki[BYK99]A335G = 1.2 nM), suggesting that the secondary amine at the restricted ring structure of BYK99 binds in a narrow region next to A33510, 24. The A335G mutation apparently provides a better fit in the binding site and can partially compensate for the increased volume of the additional methyl group in BYK73. This notion is also supported by the A335V mutant, which has largely reduced affinities for BYK99 (Ki[BYK99]A335V > 1000 nM) and SCH28080 (Ki[SCH28080]A335V > 10,000 nM). It should be noted, however, that these results do not necessarily require that the methyl group of bound BYK73 replaces the side-chain methyl of A335 in the A335G mutant.
Proposed model of P-CAB binding pocket on H+,K+-ATPase
Based on the present as well as previous results, we suggest a model for the P-CAB binding pocket of H+,K+-ATPase (Fig. 3). From EM analysis and homology modelling, we were able to define the molecular conformation of gastric H+,K+-ATPase and the binding position of the P-CAB BYK99 within the luminal-facing cavity. Based on our mutagenesis data, amino acids contributing to the P-CAB binding site were mapped in the model. These amino acids were distributed in M2, M4, M5, and M6, and surrounded the cavity facing the gastric lumen, which is consistent with the proposed P-CAB binding position (Fig. 2D,E). The location of the binding site was also consistent with mutants that do not affect P-CAB affinity (Table S3). Our cryo-EM analysis and mutagenesis data suggest that the imidazo[1,2-a]pyridine ring aligns between the M2 helix (Table 1) on one side and A335 in the M4 helix on the other side. A similar location for the imidazo[1,2-a]pyridine class of inhibitors, such as SCH28080 and BYK99, was proposed in previous studies24 that also fits the cryo-EM density presented here. In that proposed model, the imidazo[1,2-a]pyridine ring is fitted similarly in the luminal vestibule, but the para position of the phenyl group faces toward TM1, thus supporting the known mutational effects on binding as well as the structure-activity relationships given by synthetic modification of the imidazo[1,2-a]pyridine ring25, and the photoaffinity labelling within the TM1/TM2 segment of H+,K+-ATPase given by a radioactive para-azidophenyl analogue of SCH2808026. Future studies with higher-resolution cryo-EM or X-ray crystallographic analysis is required to specify the detailed molecular orientation of the P-CABs for discrimination of these binding site models.
Electron crystallographic analysis
Two-dimensional crystallization and structural analysis of the BYK99-bound E2BeF structure by electron crystallography were performed as described previously10. Briefly, a purified membrane fraction from pig stomach27 was solubilised with octaethylene glycol monododecyl ether, mixed with dioleoyl phosphatidylcholine, and dialysed against buffer containing 10 mM propionate, 10% glycerol, 1 mM BeSO4, 4 mM NaF, 100 μM BYK99, and 3 mM dithiothreitol at 3 °C for ~2 weeks. The carbon sandwich method28 was applied for the cryo grid preparation and data were collected by cryo-EM with a liquid helium-cooled stage operated by 300 keV (JEM-SF3000F)29. Micrographs were analysed using MRC image processing programs30,31,32.
Homology models of the SCH28080- or BYK99-bound H+,K+-ATPase in the E2BeF state were built with MODELLER v9.733, using the atomic model of ouabain-bound Na+,K+-ATPase (PDB ID: 4HYT)28 as a starting template. The initial manual fitting of the homology model into the density map was followed by adjustments for each individual domain and the TM helices within the EM density map using SITUS34. After the positional search, further fine fitting and connecting the split loop region was performed manually using COOT35 with regularisation refinement. Figures were prepared using UCSF Chimera36.
Chemical synthesis of SCH28080 derivatives
SCH28080 and its derivatives were synthesised according to Kaminski et al.25.
Expression of recombinant H+,K+-ATPase
The cDNA encoding the pig WT or mutant H+,K+-ATPase α-subunit and WT β-subunit were independently cloned into the BacMam vector37. The pig H+,K+-ATPase was expressed using baculovirus-mediated transduction of mammalian HEK293S GnT1- cells, as described previously15. Membrane fractions were prepared by breaking cells with a Teflon homogeniser as described previously19 and used for the following ATPase assay.
Determination of K i for SCH28080 by 96-well format ATPase assay
Before measuring the ATPase activity, the membrane fraction (4 mg/ml) was permeabilised by incubating 10 mM HEPES/Tris, pH 7.0, 10% glycerol, and 0.1% β-Escin for 10 min at room temperature to make substrates and inhibitors fully accessible, and then diluted 10 times on ice with 250 mM sucrose and 0.5 mM EGTA/Tris, pH 7.6, to stabilise the enzyme for a minimum of one day, based on the H+,K+-ATPase activity38. Permeabilised membrane fractions (~2 μg total protein/80 μl) were suspended on ice in buffer comprising 40 mM PIPES, pH 7.0, 2 mM MgCl2, 2 mM ATP, and 0–30 mM KCl in the presence or absence of the indicated concentrations of SCH28080, BYK99, or other derivatives in the 96-well plate. Reactions were initiated by incubating at 37 °C using a thermal cycler, and maintained for 1 to 5 h (depending on the activity). Reactions were terminated by withdrawing 40 μL from the 80 μL reactant, and mixing with 80 μL of stop solution comprising 6% ascorbic acid and 2% ammonium molybdate in 1 N HCl, followed by the addition of 120 μL of 2% sodium arsenate, 2% sodium citrate, and 2% acetic acid. The amount of released inorganic phosphate was determined colorimetrically39 from absorbance at 850 nm by the microplate reader (TECAN).
Data measured from the 96-well plate contained triplicates of four different sets of K+-dependent ATPase assays in the absence or presence of three different concentrations of inhibitor to give 96 data points. Data were corrected for background values in the absence of K+ at each inhibitor concentration and fit by using simultaneous nonlinear regression (global fitting)16
where: v is the ATPase activity, Vmax is the maximal ATPase activity, Km is the Michaelis constant for K+, Ki is the inhibitor constant, [S] is the K+ concentration, and [I] is the inhibitor concentration. Data were fitted by GraphPad Prism to obtain the mean and SEM.
Some of the mutants exhibited unusually high H+-ATPase activity, which is the reaction rate responsible for the spontaneous E2P dephosphorylation in the absence of K+ (i.e., basal activity). In the case of WT or most of the mutants, H+-ATPase activity was less than 5% of the total H+,K+-ATPase activity, having only a negligible effect on the determination of Ki. In some mutants, however, significant amounts of H+-ATPase (>20% of the total H+,K+-ATPase activity) led to an underestimation of Vmax value in the absence of P-CABs. For this reason, the Ki value of the mutants with high H+-ATPase activity could not be determined by global fitting. In these cases, we determined the Ki value (defined in this manuscript as Ki’), from the K m /V max plot19. These two procedures for the determination of Ki are essentially the same16, as we confirmed for the WT enzyme with SCH28080 (Ki (global fitting) = 150 nM, Ki’ (K m /V max plot) = 110 nM).
The EM density map has been deposited in the EMDataBank, http://www.emdatabank.org/ [accession code EMD-6799]. The homology model of (BYK)E2BeF has been deposited in the Protein Data Bank, http://www.pdb.org (PDB ID code 5Y0B).
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This work was supported by Grants-in-Aid for Scientific Research (B), Young Scientists (A); Platform for Drug Design, Discovery, and Development from MEXT; and Core Research for Evolutional Science and Technology from JST (JPMJCR14M4) (to K.A.); Grants-in-Aid for Young Scientists (A) (to J.S.); Grants-in-Aid for Scientific Research (C) (to K.T.); and Grants-in-Aid for Scientific Research (S.) from MEXT; the Japan New Energy and Industrial Technology Development Organization (NEDO), and the Japan Agency for Medical Research and Development (AMED) (to Y.F.). K.A. and J.S. gratefully acknowledge Ms. Mayumi Taniguchi for technical assistance, and graduate students in the Graduate School of Pharmaceutical Sciences, Nagoya University, for their contribution at the initial stage of this work. Research reported in this paper was also supported by the National Institute of Diabetes and Digestive and Kidney Diseases of the U.S. National Institutes of Health under award number 1R01DK105156 and by Biomedical Laboratory and Clinical Science Research and Development Services of the U.S. Department of Veterans Affairs under Merit Award 2I01BX001006.
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