Divalent cations Cu2+ and Zn2+ can prevent the viral growth in mammalian cells during influenza infection, and viral titers decrease significantly on a copper surface. The underlying mechanisms include DNA damage by radicals, modulation of viral protease, M1 or neuraminidase, and morphological changes in viral particles. However, the molecular mechanisms underlying divalent cation-mediated antiviral activities are unclear. An unexpected observation of this study was that a Zn2+ ion is bound by Glu68 and His137 residues at the head regions of two neighboring trimers in the crystal structure of hemagglutinin (HA) derived from A/Thailand/CU44/2006. The binding of Zn2+ at high concentrations induced multimerization of HA and decreased its acid stability. The acid-induced conformational change of HA occurred even at neutral pH in the presence of Zn2+. The fusion of viral and host endosomal membranes requires substantial conformational changes in HA upon exposure to acidic pH. Therefore, our results suggest that binding of Zn2+ may facilitate the conformational changes of HA, analogous to that induced by acidic pH.
Influenza viruses belonging to the family Orthomyxoviridae comprise four antigenic types: A, B, C, and, D. Influenza A and B viruses co-circulate and cause seasonal epidemics, and influenza C virus causes severe disease in children1,2. Based on the antigenicity of hemagglutinin (HA) and neuraminidase (NA), 18 HA and 11 NA subtypes of influenza A viruses have been identified in wild waterfowl, and subtypes H17N10 and H18N11 have been discovered in bats 3,4. The various subtypes are divided into two groups, group 1 (including H1, H2 and H5) and group 2 (including H3 and H7). Thus far, three HA (H1, H2, and H3) and two NA (N1 and N2) subtypes have adapted to humans to produce pandemic (pdm) and seasonal influenza A viruses5. The dynamic nature of influenza viral infections, particularly due to the variation of HA, remains a big challenge in minimizing the mismatch between circulating seasonal strains and vaccines.
Progression of viral particles from early to late endosomes results in large conformational changes of the active form of HA that is derived from the proteolytic cleavage of HA0 precursor into HA1 and HA26,7. The HA structure has two distinct regions. The head region is composed of the receptor binding and vestigial esterase domains of HA1, whereas the stem region includes a long central helix of HA2. The HA plays a critical role for acidic pH-induced membrane fusion in viral fitness8,9 and involves the dissociation of the head regions and the extension of central coiled-coil domains in the stem regions. In this context, the stability of HA is an important attribute of influenza viral fitness, which regulates and enhances viral growth and pathogenesis10,11. The stability of HA is changed significantly within and among the subtypes10,12, and the recent A(H1N1) 2009pdm viruses evolved to exhibit significantly more stable HA as they became seasonal strains circulating globally13,14. Mutations in the coiled coil region of HA2 and at the interface between HA1 and HA2 subunits influence the stability of HA15,16,17,18. We also demonstrated that the recombinant HA derived from A/Korea/01/2009, a 2009pdm isolate, is a monomer in solution and crystals, where HA molecules are arranged in a head-to-head manner19. However, the monomeric HA has a significantly lower stability than the trimer.
The influenza A viruses contain a significant number of Zn2+ ion20. The Zn2+ is shown to bind to M1 protein with a tetrahedral coordination with two Cys and two His residues, where the Zn2+ ion may play a structural role21. Cu2+ and Zn2+ ions, albeit less effective in the latter, significantly reduced the influenza viral titers in MDCK cells and on a copper surface22,23. Zn2+ is also an important cofactor of many viral proteins, including nucleocapsid protein 7 of HIV-1, NS3 of hepatitis C virus, VP30 of Ebola virus, E7 of human papilloma virus, VP6 of rotavirus, and E protein of Semliki Forest virus24,25,26,27,28, mainly showing a structural role in zinc binding motifs. However, our understanding of the molecular mechanisms of divalent cation-mediated antiviral activities is far from complete. In this study, solving the crystal structure of HA derived from A/Thailand/CU44/2006 (CU44) led to a surprising finding of a divalent cation Zn2+ bound to the head regions of two neighboring trimers. The divalent cation in the crystal structure appeared to enhance the stability of HA, but significantly decreased the melting temperature Tm of the CU44 HA, depending on the Zn2+ concentrations. The acid-induced conformational change of HA occurred even at neutral pH in the presence of Zn2+. Therefore, our results suggest that binding of Zn2+ may facilitate the conformational change of HA, analogous to that induced by acidic pH. Here, we report the structure of HA bound to Zn2+ ions and the effects of the divalent cation on pH-dependent conformational changes of HA.
Structure of Cu44 HA with Zn2+ ion
We originally aimed to improve the stability of HA in solution and crystals to allow high resolution analyses of how pH-induced conformational changes affect its biological functions. A total of nine mutants of the CU44 HA wild-type were constructed: L69S, I71S, L156S, I184S, F260A, and A276T of HA1 in the head region, and L73S, M77I, and V91I of HA2 in the stem region (based on H3 numbering). The mutations largely accounted for reduced exposure of hydrophobic amino acid residues on the surface and increased hydrophobic residues at the monomer–monomer interface within the trimer. They were expressed in insect cell culture, purified, and characterized by differential scanning fluorimetry (DSF). No improvement in protein stability was seen in terms of melting temperature (Tm).
We attempted to determine the crystal structure of the CU44 HA wild type as a control, by molecular replacement using PDB 4EDB as a template. The structure in space group C2 (a = 215.7 Å, b = 124.3 Å, c = 214.5 Å, b = 102.9°) was refined at 3.2 Å resolution with an R/Rfree of 26.3/29.5 and exhibited good overall geometry (Table 1). The HA trimers adopt an alternating up-and-down arrangement with head-to-head interactions (Fig. 1A). Surprisingly, anomalous difference Fourier maps calculated with phases from a model showed a pronounced peak at the head-to-head interface between two neighboring HA trimers, clearly visible at the 7 σ level (Fig. S1). Fluorescence scans around the anomalous edges using the HA crystals strongly suggested that Zn2+ ion could contribute to the strong anomalous signal at the absorption edge near at 1.284 Å (Fig. S2). Despite the lack of Zn2+ in the crystallization medium, Zn2+ ion was tentatively refined with full occupancy and B-factor of 41–47 Å2 (three Zn2+ ions in the asymmetric unit). The divalent ion binds to the side chains of Glu68 and His137 from two adjacent trimers (Fig. 1B). In the final 2|Fo| − |Fc| and |Fo| − |Fc| difference Fourier maps, the divalent cation adopts an octahedral molecular geometry, mediated by the coordination with Glu68 and His137. They likely act as bi- and monodentate ligands, respectively, to the Zn2+ ion with the coordination bond lengths of 1.9–2.3 Å.
Effects of divalent cations on HA proteins
In parallel, we carried out gel shift experiments involving native polyacrylamide gel electrophoresis of the CU44 HA in the presence of various divalent cations. The Cu2+ and Zn2+ cations promoted robust multimerization of HA (Fig. 2A, upper panel). To assess whether the presence of the divalent cations can impact the stability of HA, DSF was used to measure the changes in Tm. Many divalent cation had no effect on the Tm values of the HA, whereas the Tm values in the presence of Ni2+, Zn2+ and Cu2+ were significantly reduced by 8 °C and 18 °C and could not be obtained, respectively (Fig. 2A, lower panel). When HA was treated with 0.1–1 mM Zn2+, a significant shift in the size exclusion chromatography (SEC) profile was observed. As the concentration of Zn2+ increased, multimeric forms of the HA were eluted at the void volume (Fig. 2B, upper panel). The HA protein sample was filtered through a 0.22 μm membrane prior to chromatography and the peak at the void volume in the SEC profile became lower as the Zn2+concentration increased, suggesting that larger aggregates of HA formed at high concentrations of Zn2+. In contrast, the HA protein also induced multimerization at acidic pH, but not to the extent of formation of the larger aggregates induced by Zn2+ (Fig. 2B, lower panel). Additionally, the multimerization of the HA by Zn2+ was not abolished by the treatment of ethylenediaminetetraacetic acid (EDTA) at concentrations of 1–10 mM (Fig. S3). The conformational changes and multimeric associations of HA induced by Zn+2 or acidic pH have been examined using SEC-MALS and binding of antibodies (Fig. 2C, D). The molecular weights of HA multimers induced by Zn+2 or acidic pH were 1785 or 2039 kDa, respectively, corresponding to the associations of approximately 9 HA trimers, and the HA multimers induced by Zn+2 showed a relatively polydisperse population. In addition, the conformations induced by Zn+2 or acidic pH were not recognized by CR9114, but by the D2 interface antibody that binds to the head domain (Fig. 2D)29. The results indicate that the stem conformations of HA induced by Zn+2 or acidic pH are not recognized by CR9114 and do not represent the native prefusion conformations. Our results thus suggest that the treatment with Zn2+ induces the conformations of HA, similar to those induced by acidic pH.
Comparison of the amino acid sequences of HA from different subtypes of influenza viruses revealed the conservation of the Zn2+ binding residues, Glu68 and His137, in H1 strains, but not in other subtypes (Table 2). In some strains, including the 1918pdm and the 1933–1936 seasonal strains, the corresponding amino acid residues of HA were substituted with Asp or Tyr, respectively. Nevertheless, the unique binding of Zn2+ to HA in a broad range of H1 subtype influenza A viruses reveal a subtype-specific interaction of HA with Zn2+.
pH-dependent conformational changes of CU44 HA
Acidic pH in the endosome induces a large conformational change of HA whose stability to an activation pH is necessary for influenza virus pathogenicity and transmissibility6,7,8,9,14. In order to examine the pH-dependent stability of the CU44 HA, DSF experiments were carried out by incubating the HA at different pH conditions followed by rapid neutralization. Two distinct Tm values were obtained for the CU44 HA, 58 °C at pH 5.9–7.0 and 56 °C at pH 5.0–5.7 (Fig. 3A, upper panel). In comparison, the conformational changes started to occur at pH 6.0 upon a 10-min incubation without neutralization, with the changes occurring at pH < 6.0 being irreversible (Fig. 3A, middle panel). The Tm values continuously decreased from 52 °C at pH 5.9–5.6 to ~ 40 °C at pH 5.0. Upon a 24-h incubation, two distinct conformations were apparent, with Tm values at 58 °C at pH 7.0 and 48 °C at pH below 6.0 (Fig. 3A, lower panel). We postulate that these two distinct conformations correspond to pre- and postfusion states of the CU44 HA and its transition from a reversible to irreversible conformations occurs at pH 5.6–5.8.
Effects of Zn2+ on conformational changes and proteolytic activation of HA
To study the effect of Zn2+ on the pH-dependent stability of the CU44 HA, the HA protein was incubated with Zn2+ ion for 10 min followed by rapid neutralization at different pH conditions. Stepwise multimerization of HA proteins was observed as the pH decreased, reaching complete multimerization at below pH 5.4, whereas it occurred readily in the presence of Zn2+ even at neutral pH conditions (Fig. 3B). More pronounced multimerization was evident at higher concentrations of Zn2+. In addition, the increased concentration of Zn2+ reduced the Tm values of the HA even at neutral pH in a concentration-dependent manner (Fig. 3C). The Tm values decreased from 58 to 54 °C. Thus, the conformational changes of the HA induced by Zn2+ were similar to that occurring upon acidic incubation without neutralization, which occurred more readily as the concentration of Zn2+ increased.
Infectivity of influenza viruses depends on cleavage activation of the HA precursor into HA1 and HA2 by host proteases30. We characterized pH-dependent proteolytic activation of the CU44 HA using SDS-PAGE. The HA1 subunit was completely degraded at a pH below 5.8, as it was highly susceptible to trypsin cleavage after the acid-induced conformational change (Fig. 3D). At 1 mM Zn2+, the CU44 HA exhibited greatly enhanced susceptibility to proteolytic degradation even at neutral pH, similar to that induced by acidic pH.
Effects of Zn2+ on HA wild-type and mutants
Although the thermal stability of HA was significantly reduced by Zn2+ and the crystal structure was determined at 3.2 Å resolution, the N-linked glycan structure was exceptionally well-defined in the 2|Fo| − |Fc| electron density maps, which is unusual in HA structures. It showed a branched sugar chain of up to six monosaccharide units attached to Asn residues of the head region (Figs. 4, S4). The glycans attached to Asn54 and Asn87 are much closer to the Zn2+ binding site than other glycans in the head region, suggesting fairly stable conformations. In addition, the multimerization of glycosylated or deglycosylated HA induced by Zn2+ was not prevented by the treatment of EDTA (Fig. S3, upper and middle panels).
In order to examine the effects of Zn2+ on biophysical properties of HA, single and double mutations at the Zn2+ binding site were introduced: the H137A single mutant displayed the essentially identical Tm of the wild-type in the absence of Zn2+ and the same changes in Tm in the presence of Zn2+ (Fig. S5). The incubation of Zn2+ with the mutants induced pH-dependent conformational changes similar to those of the wild-type, where high concentrations of Zn2+ equally promoted multimerization of the mutants, similar to those produced by the wild-type (Figs. S3 and S5, lower panels for the E68A/H137A and H137A mutants, respectively). Therefore, the HA, already transformed into the postfusion conformation at high concentrations of Zn2+, is not blocked by the mutation or EDTA treatment. When the purified HA crystallized at 10–20 mg/ml by mixing with an equal volume of precipitant solution, protein crystals were produced at less than 0.4 mM Zn2+, whereas precipitates were found at higher than 0.4 mM. No crystals or precipitates were found at 0 mM Zn2+ (data not shown). Taken together, our results suggest that Zn2+ binding to HA has two phases: Zn+2 binds specifically to the head regions of HA at low concentrations, whereas, at high concentrations, it binds nonspecifically to HA, causing conformational changes similar to those induced by acidic pH.
HA is a highly dynamic molecule capable of mediating a pH-dependent transition from a prefusion to postfusion state during virus entry. Induction of irreversible conformational changes upon acidification results in the formation of a stable postfusion state via a spring-loaded mechanism31. The prefusion conformation of HA is metastable, and the receptor binding head region acts as a clamp to keep the stem region in its metastable prefusion state at neutral pH. Acidification shifts the dynamic equilibrium of HA that favors the progression of membrane fusion31. We initially constructed nine mutants to improve the stability and quality of HA in solution and crystals, and the wild-type HA crystal structure derived from A/Thailand/CU44/2006 was determined as a control. Surprisingly, the highest peak in the anomalous difference electron density maps was located at the head domain at the inter-trimer interface, which was tentatively identified as Zn2+, based on native gel electrophoresis and absorption-edge fluorescence scan results.
The Zn2+ divalent cation is essential for life, although excess Zn2+ is toxic to the cells, possibly due to its inhibition of key enzymes32. Zn2+ is involved in many biological processes including infection of a variety of microbial and viral pathogens. During the infection, the innate immune system controls the concentration of Zn2+ to prevent the growth of pathogens33. Zn2+ was present in influenza virions and binds to M1 protein20,21. In addition, the titers of influenza viruses were significantly reduced by adding Zn2+ in MDCK cells22. The mode of inhibition by Zn2+ against influenza viruses was investigated in the context of DNA damage by radicals, viral protease or neuraminidase inhibition, or morphological changes of virions21,22. However, the molecular mechanism of divalent ion-mediated inhibition of influenza viruses is not well understood.
In the crystal structure, the HA trimers line up in an alternating up and down orientation with head-to-head interactions, where Zn2+ is bound between two adjacent HA trimers. This divalent cation may be acquired from the PEG 2000 used in crystallization or the medium of insect cells. In aqueous solution, Zn2+ can be coordinated with up to six water molecules, but it is usually tetrahedrally coordinated in zinc finger proteins and enzymes34. The coordination geometry of four or five coordination to Zn2+ is applied to catalysis with high Lewis acidity, whereas it is rarely hexacoordinated in catalytic binding sites35,36. In the HA structure, the carboxylic oxygen atoms of Glu68 and imidazole nitrogen atoms of His137 are directly coordinated to the divalent cation, which results in a distorted octahedral, six-coordination geometry, involving bidentate interactions of carboxylic groups. The Zn–O and Zn–N bond lengths are from 2.0 to 2.2 Å. The mean Zn–O and Zn–N distances from octahedral structures in the Cambridge Structural Database and aqueous solution are 2.10–2.11 Å35.
The amino acid residues, Glu68 and His137, coordinated to Zn2+ are highly conserved in a broad range of H1 subtypes, although they are substituted with Asp or Tyr, respectively, in the early 1918 pandemic and the seasonal 1933–1936 strains, and not conserved in other subtypes and type B (Table 2). It is likely that the Zn2+ binding has evolved to play a structural role in the H1 subtype viruses for the past 80 years. Moreover, it was previously suggested that the acid stability of HA during membrane fusion regulates interspecies adaptation of the influenza viruses37, in which the HA acid stability affects pathogenicity with pandemic capability. In this context, the arrangement of the HA trimers with head-to-head interactions in the HA-Zn2+ complex is unique, and the Zn2+-induced conformational changes of HA equivalent to those upon acidification are very striking. Recent analyses revealed that acidification and receptor binding shifts the dynamic equilibrium of HA in favor of forward progression to membrane fusion, and either receptor binding or the presence of a target membrane promotes HA2 conversion to the postfusion state38. Similarly, enhanced interactions of the head regions by the presence of Zn2+ at low concentrations can provide an efficient way of stabilization of HA, whereas high concentrations of Zn2+ induces significant conformational changes of HA, which may result in clustering of the HA molecules, analogous to receptor-promoted formation of the postfusion conformations.
Cloning and baculovirus production of HA
The recombinant HA protein derived from A/Thailand/CU44/2006 (CU44) was produced in insect cells using recombinant baculovirus expression vectors, and the vector was constructed in previous work39. The synthesized cDNA of the CU44 wild-type HA after RNA extraction was amplified using polymerase chain reaction (PCR). The wild-type HA gene (1-503 of HA0 based on H3 numbering) was cloned into pFastBac HT A (INVITROGEN, Carlsbad, CA, USA) downstream of the gp67 secretion signal sequence of the transfer vector pAcGP67A (BD BIOSCIENCES, Woburn, MA, USA). The cloned construct had residues 18–344 (1-326) (HA1) and 345–520 (1-176) (HA2), with a thrombin cleavage site, foldon domain, and 6 × His-tag downstream of the HA gene sequence. The recombinant HA protein contained additional plasmid-encoded residues ADPG and RSLVPR at the N- and C-terminus, respectively. Mutant HA genes were prepared by site-directed mutagenesis using a pair of complementary oligonucleotides containing the H137A mutation in the gene (MACROGEN, Seoul, Korea). Briefly, ten cycles of PCR was performed with mutant oligonucleotides to amplify the mutant HA gene, which was treated with Dpn1 (NEB, MA, USA) to remove wild type HA genes for 1 h at 37 °C. Plasmids encoding the mutant HA gene (H137A) was transformed and amplified in Escherichia coli strain DH5α and the recombinant bacmid was generated according to the Bac-to-Bac expression system protocol (INVITROGEN). The sequences were confirmed by automated sequencing (MACROGEN, Seoul, Korea). The CU44 HA in this study showed three mutations different from the original CU44 HA: HA1 M116I and HA2 I91V and N169S, which was used as a wild-type. These mutations also exist in nature. Spodoptera frugiperda insect cells were transfected with the recombinant bacmid using Cellfectin II (INVITROGEN), which were harvested at 72 h post-transfection and centrifuged at 2000 rpm for 15 min to obtain baculovirus, expressing recombinant HA in the supernatant. The transfection efficiency was confirmed by PCR after extraction of DNA from 400 μl of virus.
HA protein purification
Baculovirus containing the CU44 HA wild-type or mutant (H137A) gene was used to infect suspension cultures of Hi5 cells, as described previously39. After 3 days at 28 °C, the culture medium was harvested. After centrifugation at 4000 rpm for 30 min, the supernatant was applied to a nickel–nitrilotriacetic acid (Ni–NTA) affinity column (QIAGEN, Hilden, Germany) equilibrated with 20 mM Tris–HCl, pH 8.0, and 100 mM NaCl. The column was washed with buffer containing 30 mM imidazole, and the precursor HA protein was eluted in an imidazole gradient (30–400 mM). The eluted fractions were dialyzed against 20 mM Tris–HCl (pH 8.0) and 20 mM NaCl, and hydrolyzed by TPCK-treated trypsin for 4–5 h at 4 °C for cleavage of HA0 into HA1 and HA2 and removal of the foldon and 6 × His-tag. The active form of HA was purified using Superdex 200 10/300 GL size exclusion chromatography in 50 mM Tris–HCl (pH 8.0) and 100 mM NaCl, connected to an ÄKTA FPLC system (GE Healthcare, Buckinghamshire, UK). It was concentrated in an Amicon 10,000 MWCO concentrator (Merck Millipore, Billerica, MA, USA) to 10 mg/ml for characterization and crystallization.
Cloning, expression, and purification of Endo H
The synthesized cDNA encoding for endo-β-N-acetylglucosaminidase H (Endo H), a glycohydrolase secreted by Streptomyces plicatus40, was cloned into the PMAL-p2 plasmid and transformed into Escherichia coli BL21 (DE3) (INVITROGEN, Carlsbad, USA). The cells after 0.4 mM IPTG induction were harvested by centrifugation, sonicated, and centrifuged at 12,000×g for 20 min. The supernatant containing the Endo H was purified by affinity and size exclusion chromatography using amylose (NEB, MA, USA) and Superdex 200 10/300 (GE HEALTHCARE, Uppsala, Sweden) columns, respectively. Using the purified Endo H, HA samples were treated at 0.5 μg/ml in phosphate buffer (pH 6.8) at 4 °C for 30 h and separated from the Endo H using a 10 kDa MW cutoff membrane (MERCK MILLIPORE, Billerica, MA, USA). Deglycosylation of HA by the Endo H was determined by gel-shift assays.
Native polyacrylamide gel electrophoresis (PAGE)
The purified proteins were prepared under native condition (mixed with 5 × loading buffer, 312.5 mM Tris–HCl (pH 6.8), 50% glycerol, and 0.05% bromophenol blue, without β-mercaptoethanol and sodium dodecyl sulfate). The HA wild-type or mutant (2–5 µg) was incubated in 100 mM HEPES or MES and 100 mM NaCl at different pH and 25 °C for 1 h. Electrophoresis was carried out in 25 mM Tris–HCl buffer (pH 8.8) and 192 mM glycine at 200 V and 80 mA for 1 h.
For a gel shift assay of divalent cations, the CU44 HA was mixed with 5 mM Li+, NA+, K+, Mg2+, Ca2+, Fe2+, Co2+, Ni2+, Cu2+, and Zn2+ ions in 20 mM Tris–HCl (pH 8.0) and 100 mM NaCl overnight. For HA-Zn2+ complexes, the CU44 HA was mixed with Zn2+ in 0–1 mM in 20 mM Tris–HCl (pH 8.0) and 100 mM NaCl overnight, which was then incubated in 100 mM MES-HEPES at pH 7.4, pH 6.0, pH 5.9, pH 5.8, or pH 5.4 at room temperature for 1 h. It was either recovered to neutral pH by mixing with 2 M Tris–HCL (pH 8.5) after 10 min, or incubated further for 24 h. The samples were submitted for native PAGE. In the case of the EDTA treatment, the HA-Zn2+ complex was incubated in 1 mM or 10 mM EDTA for 1 h or overnight. The electrophoresis was carried out in 25 mM Tris–HCl buffer (pH 8.8) with 192 mM glycine at 200 V and 80 mA for 1 h. The gels were stained using Coomassie Brilliant Blue R-250 (SIGMA-ALDRICH, St. Louis, MO, USA).
Size exclusion chromatography and multi-angle light scattering (SEC-MALS) analysis
The elution shift of the CU44 HA-Zn2+ complex was examined by mixing the CU44 HA with 0–1 mM Zn2+ in 20 mM Tris–HCl (pH 8.0) and 100 mM NaCl overnight. Each sample was applied to a Superdex 200 GL column (GE HEALTHCARE) equilibrated with 50 mM Tris (pH 8.0) and 100 mM NaCl at a flow rate of 0.5 ml/min, connected to a UFLC system (SHIMADZU, Kyoto, Japan). Light scattering and refractive index were measured using in-line WYATT-787-TS miniDAWN TREOS (WYATT Technology, Santa Barbara, CA, USA), and the data were analysed by Astra 6 software.
HA recognition by antibodies using ELISA
CU44 HA was incubated with 1 mM Zn2+ or 100 mM MES (pH 5.5) for ELISA at 4 °C overnight. The 8-well strip was coated with the native, Zn2+, or acidic-pH incubated CU44 HA in a total volume of 100 µl (2 ng/µl) in microplates (Corning). Following blocking with 1% BSA and PBS washing, primary antibodies (the stem-specific CR9114 or head-specific D2 H1-1/H3-1) were applied at 400, 80, 1, 3, 0.64, 0.128, and 0.026 ng per well at 37 °C for 1 h. They were then washed with PBS, and detected by anti-human IgG1-HRP (Abcam, Cambridge, UK) as the secondary antibody for 1 h. 150 µl of 3,3′,5,5′-tetramethylbenzidine (Sigma-Aldrich) was used as substrate and the reaction was stopped by the addition of 2 N sulfuric acid, and the absorbance at 450 nm was monitored.
DSF was used to measure the shift in transition temperature of HA at different pH conditions, using Stratagene MX3005P (AGILENT TECHNOLOGIES, Santa Clara, CA, USA). The reaction mixture (25 µl) containing 5 µg of the HA wild-type or mutant, 5X SYPRO Orange (INVITROGEN), 100 mM HEPES or MES and 100 mM NaCl was incubated at different pHs at 25 °C for 1 h. Temperature increment at the rate of 0.5 °C every 30 s for 50 min and relative fluorescence units were recorded at the excitation and emission wavelengths of 492 nm and 610 nm, respectively. The transition temperature was calculated from the maxima of the first derivative of relative fluorescence units/temperature using MxPro QPCR Software.
Trypsin digestion for protease susceptibility
For proteolytic cleavage analysis, the CU44 HA was mixed with Zn2+ in 0–1 mM in 20 mM Tris–HCl (pH 8.0) and 100 mM NaCl overnight, which was then incubated in 100 mM MES-HEPES at pH 7.4, pH 6.0, pH 5.9, pH 5.8, or pH 5.4 at room temperature for 1 h. It was recovered to neutral pH by mixing with 2 M Tris–HCL (pH 8.5) and mixed with 10 µg of TPCK-Trypsin (THERMO FISHER SCIENTIFIC, Waltham, MA, USA) at 37 °C for 10 min. Each reaction was stopped by adding 5 × sample buffer and heating at 95 °C for 5 min. Aliquots were analyzed by SDS-PAGE.
Crystallization and data collection
The purified HA was concentrated to 10 mg/ml in 50 mM Tris–HCl (pH 8.0) and 100 mM NaCl, and crystallized by mixing with an equal volume of precipitant solution using the sitting drop vapor diffusion method at room temperature for 3–7 days. The precipitant solution contained 0.1 M Tris–HCl, pH 7.25, 20% PEG 2000 and 2% dimethylsulfoxide used as additive. After a week, small crystals were obtained. Diffraction data were collected with the crystals flash-cooled at 100 K in a stream of liquid N2 in the mother liquor containing 10% ethylene glycerol using synchrotron radiation sources at beamlines BL-17A at photon factory (Tsukuba, Japan) and 11C at Pohang Light Source-II (PLS-II), Korea. The crystals of HA-Zn2+ complex were diffracted to 3.4 Å resolution, which belong to space group C2 with unit cell dimensions of a = 215.7 Å, b = 124.2 Å, c = 214.5 Å, a = 90°, b = 102.9°, and c = 90° (Table 1). All data were processed and scaled using the XDS41.
Structure solution and refinement
The crystal structure of the CU44 HA-Zn2+ complex was determined by molecular replacement using the CU44 HA structure (PDB ID 4EDB) as a template using PHENIX42. The initial solution was optimized by rigid body refinement, which produced interpretable electron density maps for the overall structure. Manual adjustment of the backbone and side chains was conducted and crystallographic refinement was carried out using the PHENIX program42. Difference Fourier maps, 2|Fo| − |Fc| and |Fo| − |Fc|, were used to model the active site or loop regions. After a few rounds of model rebuilding, water molecules were added using the |Fo| − |Fc| map peaks above 3.0 σ. The Rfree value was used as an indicator to validate the water picking and refinement procedure and to guard against possible overfitting of the data43. An anomalous difference Fourier map was generated to locate the position of Zn2+ ion, and Polder omit maps for different regions were generated44. The final R factor and Rfree were 0.263 and 0.295, respectively. Data and refinement statistics for the HA-Zn2+ complex are presented in Table 1. Stereochemical analysis of all refined structures using PHENIX42 revealed 1.6% outliers in the Ramachandran plot with 81.2% favored region among the 2577 residues. These outliers were located in the disordered loop regions.
The refined model has been deposited in the Protein Data Bank (PDB ID 6LKS).
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We wish to acknowledge the technical support from the staffs at beamline 11C at Pohang Light Source-II (PLS-II), Korea and BL-17A at the Photon factory, Japan, and thank Dr. J. Lee for providing an interface antibody gene (D2 H1-1/H3-1). This work was supported by grants from the strategy (NRF-2016R1E1A1A01942558) and by Korea Drug Development Fund funded by Ministry of Science and ICT, Ministry of Trade, Industry, and Energy, and Ministry of Health and Welfare (KDDF-201712-14).
The authors declare no competing interests.
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Seok, J.H., Kim, H., Lee, D.B. et al. Divalent cation-induced conformational changes of influenza virus hemagglutinin. Sci Rep 10, 15457 (2020). https://doi.org/10.1038/s41598-020-72368-x