Decades of intense herbicide use has led to resistance in weeds. Without innovative weed management practices and new herbicidal modes of action, the unabated rise of herbicide resistance will undoubtedly place further stress upon food security. HMGR (3-hydroxy-3-methylglutaryl-coenzyme A reductase) is the rate limiting enzyme of the eukaryotic mevalonate pathway successfully targeted by statins to treat hypercholesterolemia in humans. As HMGR inhibitors have been shown to be herbicidal, HMGR could represent a mode of action target for the development of herbicides. Here, we present the crystal structure of a HMGR from Arabidopsis thaliana (AtHMG1) which exhibits a wider active site than previously determined structures from different species. This plant conserved feature enables the rational design of specific HMGR inhibitors and we develop a tolerance trait through sequence analysis of fungal gene clusters. These results suggest HMGR to be a viable herbicide target modifiable to provide a tolerance trait.
As herbicide resistance continues to rise, the efficacy of herbicides has diminished1 such that new modes of action are desperately needed. Only one new herbicide mode of action has been brought to market in almost 40 years2. Weeds are yet to evolve significant resistance to clomazone and bixlozone1, two herbicides that disrupt isoprenoid biosynthesis by targeting the enzyme 1-deoxy-d-xylulose-5-phosphate synthase3. Found in all kingdoms of life, isoprenoid biosynthesis is crucial for the synthesis of lipids, hormones, vitamins and defence compounds4,5,6. The biosynthetic route differs between kingdoms; most animals, fungi, protists and archaea use a mevalonate (MVA) pathway, whereas most Gram-negative bacteria including cyanobacteria use a methylerythritol phosphate (MEP) pathway7. Through a shared evolutionary history with cyanobacteria, plants use both pathways7,8,9,10,11 compartmentalised to the cytosol (MVA) or plastids (MEP)12,13,14. None of the known modes of action for any of the commercial herbicides affect the MVA pathway1. An important enzyme in the MVA pathway is HMGR, which is a highly regulated15,16,17,18,19, the rate-limiting enzyme of the MVA pathway and is the target of the group of hypercholesterolaemia therapeutics known as statins20,21. Two classes (I and II) of HMGR have been defined22 based on the differences between the catalytic core domain structure23,24, the presence of an N-terminal membrane domain of between two (plants) and eight (human) membrane-spanning helices in the majority of class I enzymes20,25, and the varied NAD(P)H cofactor preference26. HMGR regulation appears to be conserved between humans and plants with the N-terminus regulated by ubiquitination whereas catalytic core activity is regulated by phosphorylation7. Many of the regulatory proteins differ, however, and this is further complicated by plants having multiple copies or isoforms plus a wide variety of external signals modifying expression, such as light and herbivory7,27.
The first potent statin inhibitor of HMGR discovered was mevastatin, isolated from Penicillium citrinum in 197628. Lovastatin, isolated from Aspergillus terreus in 1978, became the first commercial statin in 198729. Second-generation statins have been semi-synthetic or synthetic products29, but all statins competitively inhibit HMGR via a HMG-like moiety and a variable hydrophobic group that together give affinities to HMGR that are 10,000-fold higher than HMG-CoA30. Lovastatin and mevastatin, as well as the semi-synthetic pravastatin and synthetic atorvastatin are all known to be herbicidal31,32,33. HMGR might have been overlooked as a herbicide target due to potential off-target risks arising from its conservation in humans and the antimicrobial activity of statins34, but recently developed selective insecticides against HMGR illustrate the potential to develop HMGR herbicides35.
Here, we solve crystal structures for a plant HMGR in apo form and complexed with a statin. These structures reveal a wider active site conserved in plants compared to other organisms. By rational design we develop statin derivatives with over 20-fold specificity for the plant over the human enzyme and, which importantly, retain herbicidal activity. By comparing the AtHMG1 structure to fungal HMGR genes in biosynthetic clusters for natural statins, we demonstrate a single amino acid change confers statin tolerance in vitro and in planta. Together these findings suggest HMGR is a viable target for herbicide development.
Statins range in herbicidal activity
Previous studies have shown several statins to exhibit herbicidal activity against several plant species including Lemna gibba, Raphanus sativus, Scoparia dulcis and A. thaliana31,32,33,36,37. However, there is a lack of comparative data regarding the herbicidal efficacy of statins especially for second-generation, synthetic statins. To assess herbicidal activity, we treated a model dicot and a monocot (A. thaliana and Eragrostis tef, respectively) with a dose range of eight commercially available statins on soil, pre- and post-emergence (Fig. 1). All statins were more herbicidal against the dicot and in general were more effective post-emergence. In line with their physicochemical properties more closely matching those of post-emergence herbicides (Supplementary Fig. 1a). The synthetic statin rosuvastatin was the most herbicidal statin being lethal to A. thaliana at ~15 μM without formulation beyond including a wetting agent. Given that under the same conditions formulated glyphosate (Roundup®) is lethal at ~35 μM (Supplementary Fig. 1b, c), we surmised that HMGR could represent a potential herbicide target.
Crystal structure of AtHMG1 reveals scope for species selective compounds
A. thaliana has two HMGR genes with different expression patterns, but AtHMG1 (At1g76490) is the most highly epxressed38. The N-terminal transmembrane domains of HMGR are highly divergent between species and absent from class II HMGRs (Supplementary Fig. 2). By contrast, the conserved extracellular domain of AtHMG1 shares ~54% sequence identity with HsHMGCR and strictly conserved catalytic residues (Supplementary Fig. 2). To develop plant-specific statins and mitigate off-target effects, we solved the crystal structure of the core domain of apo AtHMG1 and in complex with pitavastatin to resolutions of 1.9 and 2.1 Å, respectively, in space groupI 41 2 2. Attempts were made to crystallise type I statins as described previously24; however, electron density for these ligands was ambiguous. The structure of the apo AtHMG1 displayed a single monomer in the asymmetric unit which through crystallographic symmetry forms a homotetrameric assembly (Fig. 2a), consisting of two canonical class I homodimeric HMGR folds, with high structural similarity to HsHMGCR (PDB 1HWK, r.m.s.d. 1.1 Å over 371 Cα atoms, Fig. 2b).
Closer inspection of the statin-binding pocket revealed two substitutions in AtHMG1 with respect to HsHMGCR located at the hydrophobic CoA binding region of the active site pocket39, specifically, Ile562/Leu857 and Ile389/Val683 in AtHMG1/HsHMGCR respectively (Fig. 2c, d). Furthermore, a plant conserved Val to Pro (Pro236/Val530 A. thaliana/human) substitution at the start of the Lβ1-strand is the likely cause of conformational flexibility and lack of electron density in the Nα4-Lβ1 loop adjacent to the active site-delineating Lβ2-Lα1 loop (Fig. 2e, Supplementary Fig. 3a, b and Supplementary Table 1). This flexibility results in the loss of a type II β-turn found within the HsHMGCR Lβ2-Lα1 loop that is stabilised by hydrogen bonding between a conserved Glu (Glu234/Glu528 AtHMG1/HsHMGCR) and a Cys backbone amine (Cys267/Cys561 AtHMG1/HsHMGCR) (Fig. 2f). This altered conformation of the Lβ2-Lα1 loop is not seen in any of the previous class I and II HMGR crystal structures24,26,30,40,41,42,43,44,45,46,47,48,49,50 and allows alternative conformations of the Cys267 residue (Fig. 2e, g, h). Importantly, the arrangement of the AtHMG1 Lβ2-Lα1 loop results in Glu265 being unable to form a hydrogen bond with the O5-hydroxyl group of the HMG moiety of statins or the equivalent thioester oxygen of HMG-CoA, as it is shifted 2.5 Å away, creating a wider pocket (Fig. 2g). In this orientation it is more likely that Lys397 acts as a proton donor in the catalytic reduction of HMG-CoA to mevalonate as is suggested to occur in bacteria50 and with molecular dynamics and quantum mechanics/molecular mechanics simulations with HsHMGCR51. Together, these differences increase the solvent-accessible area of the statin pocket from ~314 Å3 in HsHMGCR to ~357 Å3 in AtHMG152.
The complex of AtHMG1 with pitavastatin (Fig. 3a, b) revealed a binding mode highly similar to fluvastatin in HsHMGCR24 (Fig. 3c). Conserved polar interactions occur with the residues local to the cis loop Arg296, Ser390, Asp396, Lys397, Lys398, Asn461 (HsHMGCR Arg590, Ser684, Asp690, Lys691, Lys692, Asn755) and a salt-bridge between the terminal carboxylate of the HMG moiety with Lys441 (HsHMGCR Lys735) (Fig. 3a). The fluorophenyl group of pitavastatin maintains conserved stacking interactions with Arg296 (HsHMGCR Arg590) and hydrophobic interactions between the quinoline and cyclopropyl moiety with residues Leu268, Ile389, Leu558, Asp561 (HsHMGCR Leu562, Val683, Leu853, Asp856). This complex structure however also revealed two notable differences between the binding mode of class II statins in AtHMG1 and HsHMGCR; (i) loss of hydrogen bonding to the O5-hydroxyl group of the HMG moiety of statins from Glu265 (HsHMGCR Glu559), despite a slight shift of Glu265 towards the bound inhibitor (Fig. 3a and Supplementary Fig. 3c), and (ii) the loss of hydrophobic interactions with Gly266, His458 and Ile562 (HsHMGCR Gly560, His752 and Leu857). Unique hydrophobic contacts were made between pitavastatin and residues Ser271 and Ser367 of AtHMG1 (HsHMGCR Ser565 and Ser661).
Development of plant-specific analogues of statins
Our insights from the crystal structure of a model plant HMGR and the binding mode of pitavastatin provided the opportunity to rationally design plant-specific inhibitors. To this end, we sought to exploit the Lβ2-Lα1 loop region of AtHMG1 by developing analogues (1–9) of the more chemically tractable atorvastatin with modifications at the isopropyl group on the central pyrrole ring (Supplementary Fig. 3d). Activity of the atorvastatin scaffold against HsHMGCR was previously found to be reduced with increasing size of the alkyl substituent53 whereas the wider pocket of AtHMG1 might accommodate larger groups. In addition, the loss of interactions with O5-hydroxyl group of the HMG moiety with Glu265 could be targeted by incorporating a hydrogen bond donor (Fig. 2e, g). Thus 1–9 were synthesised (Supplementary Method 1) and assessed for herbicidal activity on soil with A. thaliana (Fig. 4a) and for species-specificity against HsHMGCR and AtHMG1 in vitro by a fluorometric, NADPH-depletion assay (Fig. 4b–d).
Overall, atorvastatin analogues with side chains of similar length had similar herbicidal and in vitro inhibitory activity to the parent, whereas side chains longer than the isopropyl group had reduced activity (Fig. 4). Compounds 4 and 7 retained herbicidal activity and displayed a preference for AtHMG1 over HsHMGCR in an initial screen (Fig. 4a, b). Dose-response curves confirmed compound 7 had switched preference from human to plant when compared to atorvastatin, showing >20-fold higher specificity for AtHMG1 (IC50 32 nM ±12 nM) over HsHMGCR (IC50 890 nM ±143 nM) in vitro (Fig. 4c, d). These molecules provide a framework for the future development of plant-specific HMGR inhibitors that might exhibit stronger herbicidal activity.
Exploiting biosynthetic gene clusters to engineer statin tolerance
The most commercially successful herbicides are often paired with a tolerance trait in crops. Statins produced from fungal biosynthetic gene clusters usually contain a copy of HMGR that imparts self-resistance54,55,56, so we sought to determine the structural basis for this resistance. Sequence alignment of a HMGR gene (lvrA) from the A. terreus genome revealed several mutations in the cluster-associated copy that were not present in the housekeeping copy (Supplementary Fig. 4). The corresponding residues of the AtHMG1 crystal structure revealed a Leu (Leu558) to Thr mutation, whose equivalent was conserved in all A. terreus genomes in the NCBI database. The Leu to Thr mutation would likely disrupt the hydrophobic pocket essential for accommodating the decalin ring of natural statins (Fig. 5a), and so was incorporated into recombinant AtHMG1. The AtHMG1-L558T mutant was resistant to a range of statins (Fig. 5b) with >20-fold resistance to rosuvastatin in vitro (WT IC50 53 nM ±20 nM, L558T IC50 >1000 nM) (Fig. 5c). Without inhibitors, AtHMG1-L558T had reduced catalytic activity (WT Km 69 µM ± 19 µM and kcat 10.7 ± 1.0 s−1, L558T Km 24 µM ±16 µM and kcat 2.4 ± 0.3 s−1) (Supplementary Fig. 5), but remained within the range of previously published rates for other class I and II HMGR enzymes57.
To validate the potential of the L558T mutation for providing a plant tolerance trait, we overexpressed full-length AtHMG1 (35 S::AtHMG1) and its equivalent with the L558T mutation (35 S::AtHMG1-L558T) in A. thaliana, using a cauliflower mosaic virus (CaMV) 35 S promoter. It has previously been shown that overexpressing AtHMG1 in A. thaliana can give rise to a 40-fold rise in mRNA levels and a modest rise in resistance to lovastatin compared to non-transformed WT controls58. Here we found with data collated from 19 independent T2 35 S::AtHMG1 lines and 14 independent 35 S::AtHMG1-L558T T2 lines that both constructs conferred similar resistance to the selectable marker hygromycin (Fig. 6a, d). However, the 35 S::AtHMG1-L558T lines were over sixfold more resistant to rosuvastatin (IC50 300 µM vs ±18 µM) than 35 S::AtHMG1 lines (IC50 46 µM ±5 µM) and more than 100-fold more resistant than non-transformed WT (IC50 3 µM vs ±1 µM) (Fig. 6b, d). Furthermore, analysis of the effects of rosuvastatin revealed 35 S::AtHMG1-L558T lines were up to 16-fold less sensitive to treatment than 35 S::AtHMG1 lines (Fig. 6c). These results illustrate the potential for HMGR to have a tolerance trait and further validates the in vitro results (Fig. 5b, c).
The relentless rise in herbicide-resistant weeds already poses a significant threat to global food security and as such, new herbicides with new modes of action are desperately needed. Moreover, as consumer attitudes shift, natural product ‘bioherbicides’ will rise in their appeal and currently in the USA enjoy an accelerated regulatory journey59.
Herein, we have validated HMGR as a potential herbicide target. Using the HMGR crystal structure from a model plant we have demonstrated that, despite its overall sequence and structure conservation with HsHMGCR, differences in the architecture (especially the active site) can be exploited to develop plant-specific synthetic HMGR inhibitors. The progress herein provides a basis for the discovery of natural product statins that might be suitable bioherbicides.
The differences in the architecture of AtHMG1 that allowed for species selectivity largely arise from an unusual orientation of the Lβ2-Lα1 loop that is likely the result of increased flexibility in the neighbouring Nα4-Lβ1 loop. The atypical orientation of the Lβ2-Lα1 loop in AtHMG1 disrupts the hydrogen bonding network formed between the catalytic residues Glu265/Lys397/Asn461/Asp473 (HsHMGCR Glu559/Lys691/Asn755/Asp767), thereby retaining only those hydrogen bonds that stabilise the catalytic Lys via the adjacent Asn and Asp residues. The conserved location of the catalytic Lys between AtHMG1 and other class I and II HMGRs strongly suggests this residue is responsible for polarising the carbonyl oxygen of HMG-CoA substrate and mevaldehyde intermediate, and for performing the final protonation step. Glu265 is not in a favourable position to hydrogen bond to either the substrate thioester oxygen or the adjacent Asp473, which based on HsHMGCR in silico simulations (HsHMGCR Glu559 and Asp767) might be expected to hydrogen bond and stabilise the mevaldyl-CoA intermediate51. Further molecular dynamics studies with AtHMG1, its substrate and cofactors might determine if the role of Glu265 is to hydrogen bond to Asp473, or to directly protonate the substrate as previous modelling studies have suggested60,61.
Here, we rationally designed a compound with >20-fold preference for plant HMGR in vitro with limited modification to the parent scaffold. Modelling of atorvastatin along with compounds 4 and 7 into the active site of HsHMGCR revealed a single dominant high-affinity binding mode with a large drop in affinity to the next most favourable binding mode. Atorvastatin exhibited the highest affinity followed by compound 7 and 4 (Supplementary Fig. 6) consistent with in vitro results (Fig. 4). Modelling with AtHMG1 revealed more varied poses of the analogues, with similar affinities between the most favourable binding modes. These binding modes are possibly facilitated by a wider active site and flexibility in the Lβ2-Lα1 loop region (Supplementary Fig. 3c) and might account for the difficulty we had in obtaining co-crystal structures for AtHMG1. The lower affinity for AtHMG1 than HsHMGCR for compounds 4 and 7 suggests further molecular dynamics simulations and crystallographic studies may be necessary to help reveal the molecular basis of in vitro specificity (Fig. 4). Notably, selectivity over HsHMGCR was also obtained by targeting the same Lβ2-Lα1 loop region in Manduca sexta using gem-difluoromethylenated HMGR inhibitors35. Similar derivatives may also prove to be selective for plant HMGRs. Overall, the developed compounds provide a framework for further structure-based rational herbicide design targeting the Lβ2-Lα1 loop region of AtHMG1, which could be validated for selectivity in mammalian in vivo studies. Greater species selectivity might be obtainable by targeting the N-terminal domain of HMGR, which is highly divergent between humans and plants and is absent from class II HMGRs. A recent crystal structure of the regulatory elements that interact with the N-terminal domain in HsHMGCR and studies of compounds that increase HMGR degradation suggest that this could be an alternative mechanism to lower cholesterol levels16,18. Future studies of the regulatory elements interacting with plant HMGR N-terminal domain and complexed crystal structures might in the same way also provide an avenue to develop more species-specific inhibitors of HMGR. The regulatory elements that control plant lipid metabolism might also provide new herbicidal targets, just as the proprotein convertase subtilisin/kexin type 9 and angiopoietin-like 3 are providing new avenues for the treatment of hypercholesterolaemia62,63.
By analysing the AtHMG1 crystal structure and sequences in fungal biosynthetic gene clusters, we identified a mutation conferring statin resistance without adversely affecting catalytic activity. Overexpressing this mutant protein in A. thaliana demonstrated its potential as a tolerance trait, but further investigations are needed. These could include (i) the efficacy of this protein mutant in different species; (ii) optimisation of expression and regulation, by modifying the N-terminal domain; (iii) its effects on sterol levels and seed set64; and (iv) determining what HMGR inhibitor residues remain in the treated crop or soil. Future studies might also focus on other residues that potentially impart resistance, such as the end region of the Sβ4 strand (residues 387–390), that show conservation in putative resistance genes from Penicillium citrinum and Xylaria grammica and could affect binding of the butyryl group of natural statins. We envisage that the development and discovery of new, natural product herbicides65,66 might also benefit from a similar approach to engineering resistance alleles from biosynthetic gene clusters containing compounds or targets of interest.
Herbicidal activity assay
Approximately 30 seeds of A. thaliana (accession Col-0) or E. tef were sown in 63 × 63 × 59 mm pots of Irish peat (Bord na Móna Horticulture Ltd, Newbridge, Ireland). Seeds were incubated in the dark for 3 days at 4 °C to synchronise germination. A single pre-emergence treatment (day 0) was performed when these seeds were transferred to a growth room at 22 °C with a 16:8 h light:dark photoperiod and 60% relative humidity. Two post-emergence treatments were performed following emergence of the seedlings (day 1) at days 4 and 7. Plants were watered accordingly throughout the experiment to maintain adequate moisture and photographed on day 16. Treatments were conducted with rosuvastatin, simvastatin, fluvastatin, atorvastatin (AK Scientific), pravastatin (BOC Sciences), lovastatin (Sapphire Bioscience), mevastatin, pitavastatin (Focus Bioscience), glyphosate, RoundUp® and atorvastatin analogues (1–9). To treat, 0.5 mL of each compound in a final concentration of 2% dimethyl sulfoxide (DMSO) and 0.02% Brushwet (SST Dandenong, Australia) was pipetted onto seedlings. Full experimental details and characterisation of atorvastatin analogue 1–9 synthesis can be found in Supplementary Method 1 and Supplementary Figs. 7–62. Growth inhibition was quantified by detecting green pixels for healthy seedlings using ImageJ (National Institutes of Health, 1.53 v) and the ‘Threshold Colour’ plug-in with the following settings: hue 50–110, saturation 125–255, brightness 30–25567. Images were converted into 8-bit format, and pixels measured over the same area. Data were normalised to a negative control to provide percentage inhibition.
HMG-CoA reductase expression and purification
An E. coli codon-optimised DNA sequence encoding the conserved extracellular region of AtHMG1 (Uniprot P14891, At1g76490, residues 121–592) was cloned into pQE30 (Qiagen) following an N-terminal His6-tag and tobacco etch virus cleavage site. The protein was expressed in the T7 SHuffle Express strain of E. coli (New England Biolabs) transformed with pREP4 (Qiagen) with the proteins expressed and purified as previously described68. Briefly, cultures were grown in lysogeny broth containing 100 μg/mL ampicillin and 35 μg/mL kanamycin at 30 °C to an OD600 of 0.8–1.0. Cells were cooled to 16 °C before the expression was induced with 0.1 mM isopropyl β-D-1-thiogalactopyranoside. Following overnight culture, cells were harvested by centrifugation and lysed by ultrasonication in 100 mM HEPES (pH 7.5), 150 mM sodium chloride, 5 mM dithiothreitol, 0.1% Triton X-100. Lysed cells were then centrifuged (15,000×g) and the supernatant was incubated in 30 mL batches with Ni-NTA resin overnight at 4 °C. The resin was then washed with 50 mL of 100 mM HEPES (pH 7.5), 150 mM sodium chloride, 5 mM dithiothreitol followed by 50 mL of 100 mM HEPES (pH 7.5), 150 mM sodium chloride, 5 mM dithiothreitol, 20 mM imidazole. The protein was then eluted with 50 mL of 100 mM HEPES (pH 7.5), 150 mM sodium chloride, 5 mM dithiothreitol, 300 mM imidazole. Eluted protein was concentrated with a 30 kDa centrifugal filter unit (Millipore) and purified by size-exclusion chromatography (HiLoad 16/600 Superdex 200) in 100 mM HEPES (pH 7.5), 150 mM sodium chloride, 5 mM dithiothreitol. The protein was assessed for purity by SDS-PAGE, and protein concentration was determined by spectrophotometry.
In vitro HMGR assay
AtHMG1 described above and human HMGR (HsHMGCR, Uniprot P04035, residues 441–888, cloned as above) were purified as above, and activity was determined by spectrophotometric measurement of the decrease in absorbance at 340 nm that occurs with NADPH oxidation in the presence of substrate HMG-CoA (Sigma-Aldrich). Reactions were performed with an assay buffer consisting of 150 mM sodium chloride, 5 mM dithiothreitol, 50 mM HEPES pH 7.4 and 2% DMSO. For kinetics determinations, a final concentration of 150 nM enzyme was incubated at 37 °C in 300 μM NADPH and different concentrations of HMG-CoA. Non-linear regression analysis was performed with GraphPad Prism 9 by plotting the initial reaction rates, v0, interpolated from a standard curve against the substrate concentration. The Michaelis–Menten constant, Km, was determined by fitting the data with a Michaelis–Menten equation and values for kcat were calculated by dividing Vmax by the molar enzyme concentration. To calculate relative specific activity, 500 nM of test compounds were pre-incubated at 37 °C with enzyme and 300 μM NADPH for 15 min before adding HMG-CoA to 200 μM. Resultant values were background subtracted and normalised to the average of the no-inhibitor control. For IC50 determinations, the same protocol was used, but varying inhibitor concentrations. Rosuvastatin data were plotted with a four-parameter (WT), and normalised response (L558T) non-linear regression model and atorvastatin and analogues were plotted with a normalised response with variable slope non-linear regression model.
Crystallisation and data collection
The C-terminal core residues of AtHMG1 (residues 121–576) were cloned and purified as above. The core domain was concentrated to 10–15 mg/mL and used immediately for crystallisation. Crystal screening was performed with 96-well Intelli-Plates (Hampton Research) with 80 μL of reservoir solution using the sitting-drop vapour diffusion method at 16 °C. Crystals were obtained with a mother-liquor of 0.2 M ammonium sulphate, 0.1 M HEPES and 35% w/v poly(acrylic acid sodium salt) 2100 from the Molecular Dimensions MIDASplusTM screen. Crystals were optimised using a 96-well additive screen, and well-diffracting crystals obtained in the same plates with a 1 μL droplet containing 0.6 μL of the above mother-liquor, 0.3 μL of protein and 0.1 μL of Hampton Research additive screen. Crystals used for inhibitor soaks were grown with the additives 40% v/v pentaerythritol ethoxylate (3/4 EO/OH) and 0.1 M iron(III) chloride hexahydrate. Inhibitor soaks were carried out in the same mother-liquor with 1 mg/mL of inhibitors. Single crystals were quickly soaked in mother-liquor containing 25% glycerol as a cryoprotectant before being flash frozen and stored in liquid nitrogen. Data collection was performed at 100 K on the Australian MX2 (micro-focus) beamline69 with 1.9 Å resolution for the apo form and 2.1 Å for inhibitor complexed AtHMG1.
Crystal structure determination, refinement and model building
Apo and complexed AtHMG1 diffraction data were processed using XDS and scaled with AIMLESS from CCP470,71. A sequence alignment of AtHMG1 and HsHMGCR was generated using ClustalO and used to create a search model of AtHMG1 based on the last common atom of PDB 1HW8. This model was then used for molecular replacement with PHASER from CCP472. Manual building and refinement were performed in iterative cycles with Coot and REFMAC5 using the CCP4 programme suite73. Structure analysis and validation were carried out with Coot and MolProbity74. The refined AtHMG1 structure was then used as a search model for molecular replacement with data from inhibitor complexed crystals. Crystallographic data and refinement statistics are summarised in Table 1 with Ramachandran plot values calculated from CCP4. Coordinates and structure factors were deposited into the PDB under accession codes 7ULI and 8ECG. Figures illustrating the structures were generated using PyMol.
In planta statin resistance assay
DNA encoding the full-length AtHMG1 protein (Uniprot P14891, residues 1–592) and the corresponding L558T mutant were cloned into a derivative of the pMDC43 binary vector75 to yield 35 S::AtHMG1 and 35 S::AtHMG1-L558T transgenes, respectively. These constructs were then introduced into Agrobacterium tumefaciens strain LBA4404 and separately used to transform A. thaliana by the floral dip method76,77. Seeds (T0/1) of transformed plants were collected and surface sterilised using 600 µL 70% ethanol, 750 µL 100% ethanol and soaked in 800 µL 50% bleach for 8 min, before washing with 800 µL sterile water and resuspension with 0.1% agar. Selection was performed on 30 µg/mL hygromycin growth medium (1% agar, 1% glucose, 0.45% Murashige & Skoog salts with vitamins, 0.3% 2-(N-morpholino)-ethanesulfonic acid (MES) (v/v), pH 5.7) in a growth room at 22 °C with 16:8 h light:dark photoperiod and 60% relative humidity. Surviving plants were transferred to 63 ×63 × 59 mm pots of Irish peat and grown to maturity in the same growth conditions. Seeds from plants with an adequate seed yield were then sterilised and selected again as described above with 30 µg/mL hygromycin growth medium. Seeds (T2) from 22 lines of 35 S::AtHMG1 and 15 lines of 35 S::AtHMG1-L558T plants that exhibited approximately 3:1 segregation ratio of hygromycin resistant:sensitive were then sown (~15 seeds/well, n = 3 replicates), along with wild-type (WT) A. thaliana, on sterile 96-well microplates with 0.25 mL/well growth medium containing a low dose range serial dilution of 8–2000 µg/mL hygromycin and of 0.16–40 µM rosuvastatin (final concentration 2% DMSO) with respective media only controls, and then again on a second higher dose range of 195–50,000 µg/mL hygromycin and of 20–5120 µM rosuvastatin (final concentration 2% DMSO). Plates were sealed with porous tape and grown for a minimum of 10 days with the growth conditions described above. Plates were then imaged, and growth quantified using ImageJ as described above. Total green pixels were normalised against negative controls for the respective lines (2% DMSO and water) to provide percentage inhibition. Three of 22 lines of 35 S::AtHMG1 and 1 of 15 lines of 35 S::AtHMG1-L558T plants were excluded from further analysis based on poor growth of the negative control or for displaying low hygromycin resistance. One of 19 35 S::AtHMG1 lines and 2 of the 14 35 S::AtHMG1-L558T lines had data only for the higher dose range of hygromycin and rosuvastatin. For IC50 determinations, all data were respectively combined from 19 lines of 35 S::AtHMG1, 14 lines of 35 S::AtHMG1-L558T and WT A. thaliana. Growth inhibition at varying concentrations of hygromycin and rosuvastatin were plotted with a four-parameter non-linear regression model using GraphPad Prism 9.
Further information on research design is available in the Nature Research Reporting Summary linked to this article.
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The authors thank Grishma Vadlamani and Yit-Heng Chooi for their helpful comments. This research was undertaken in part using the MX2 beamline at the Australian Synchrotron, part of The Australian Nuclear Science and Technology Organisation, and made use of the Australian Cancer Research Foundation detector. J.H. was supported by an Australian Research Council Discovery Early Career Researcher Award (DE180101445) and funded in part by Nexgen Plants. This work was supported by an Australian Research Council Discovery Project DP190101048 to J.S.M., K.A.S. and J.H. and an ARC Linkage Infrastructure Equipment and Facilities Grant (LE190100123) to K.A.S.
The authors declare no competing interests.
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Haywood, J., Breese, K.J., Zhang, J. et al. A fungal tolerance trait and selective inhibitors proffer HMG-CoA reductase as a herbicide mode-of-action. Nat Commun 13, 5563 (2022). https://doi.org/10.1038/s41467-022-33185-0