Tandem ketone reduction in pepstatin biosynthesis reveals an F420H2–dependent statine pathway
Jingjun Mo, Asfandyar Sikandar, Haowen Zhao, Ghader Bashiri, Liujie Huo, Martin Empting, Rolf Müller, Chengzhang Fu
TL;DR
Scientists discovered a new pathway for making pepstatins, using a special enzyme to create key statine parts.
Contribution
The study reveals a novel F420H2-dependent oxidoreductase pathway for statine biosynthesis in pepstatin production.
Findings
PepI catalyzes the tandem reduction of β-keto intermediates to form two statine residues in pepstatin.
The biosynthesis involves an unconventional gene cluster with nonribosomal and polyketide synthase genes.
Structural and mutagenesis studies identify critical residues in F420H2-dependent oxidoreductase function.
Abstract
Pepstatins are potent inhibitors of aspartic proteases, featuring two statine residues crucial for target binding. However, the biosynthesis of pepstatins, especially their statine substructure, remains elusive. Here, we discover and characterize an unconventional gene cluster responsible for pepstatin biosynthesis, comprising discrete nonribosomal peptide synthetase and polyketide synthase genes, highlighting its trans-acting and iterative nature. Central to this pathway is PepI, an F420H2-dependent oxidoreductase. The biochemical characterization of PepI reveals its role in the tandem reduction of β-keto pepstatin intermediates. PepI first catalyzes the formation of the central statine, then produces the C-terminal statine moiety. The post-assembly-line formation of statine by PepI contrasts with the previously hypothesized biosynthesis involving polyketide synthase ketoreductase…
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Figure 6- —https://doi.org/10.13039/501100002347Bundesministerium für Bildung und Forschung (Federal Ministry of Education and Research)
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Taxonomy
TopicsMicrobial Natural Products and Biosynthesis · Peptidase Inhibition and Analysis · Plant biochemistry and biosynthesis
Introduction
Pepstatins are highly potent inhibitors, effective in the pico- to nanomolar range, against various aspartic proteases (APs) such as pepsin and cathepsin D^1–5^. APs are endopeptidases discovered from all three domains of life and viruses. They are widely considered promising therapeutic targets owing to their vital roles in underlying physiological processes and the pathogenesis of various diseases. Notable examples include HIV-1 protease for HIV/AIDS, renin for hypertension, β- and γ-secretases for Alzheimer’s disease, plasmepsin for malaria, and the secreted APs for fungal infections^6^. Pepstatins are linear N-acyl pentapeptides featuring two (3S,4S)−4-amino-3-hydroxy-6-methylheptanoic acid residues, which are nonproteogenic γ-amino acids known as statines (Sta; Fig. 1a). Crystal structures of different APs in complex with pepstatins or structural analogs revealed that the central Sta residue forms hydrogen bonding with the two catalytic Asp residues^7^, vital to AP inhibition (Fig. 1b). Sta mimics the tetrahedral transition state during catalysis forming a non-cleavable structural analog of the scissile bond present in AP substrates. Insights into the inhibitory mechanism of pepstatin on APs have been instrumental in the development of peptide isostere classes of AP inhibitors^8^.Fig. 1. Representative statine-containing natural products, pepstatin binding mode, and the proposed pathway for statine biosynthesis.a Pepstatin A and representative known compounds with Sta/Sta-like residues (highlighted in red). b Interactions between pepstatin A and cathepsin D (PDB ID:1LYB). Only hydrogen bonds between pepstatin A (orange) and residues in the protein binding pocket (cyan) are shown. c The prior hypothesis on statine biosynthesis involving a modular PKS KR domain^26^.
Since the discovery of pepstatins from actinomycetes^9,10^, numerous studies have focused on their AP-inhibitory activity and mechanism. However, the pepstatin biosynthetic pathway has remained unclear. Pepstatins contain a Val-Val-Sta-Ala-Sta pentapeptide decorated with a variable N-terminal acyl chain^2,10,11^. The Sta residues in the pepstatin-like ahpatinins may be replaced by 4-amino-3-hydroxy-5-phenylpentanoic acid but retain the 3-OH-4-NH_2_ feature^12,13^. A feeding study using ^14^C-labeled compounds suggested the Sta residues in pepstatin are derived from l-leucine and malonate^14^. The Sta or Sta-like residues with the 3-OH-4-NH_2_ framework are also found in other natural products (representative examples in Fig. 1a)^15–25^. The biosynthesis of these substructures has been hypothesized to involve a collaborative process between nonribosomal peptide synthetase (NRPS) and polyketide synthase (PKS) modules^26^. In this proposed pathway, an NRPS module activates an α-amino acid such as leucine and loads it to the cognate peptidyl carrier protein (PCP) domain. The acyltransferase (AT) domain then attaches the malonyl-CoA extending unit to the acyl carrier protein (ACP) domain. A Claisen condensation reaction leads to the extension of the peptidyl thioester, forming a β-keto ester. In the didemnin biosynthetic gene cluster (BGC)^27^, isoleucine is activated, and the ketoreductase (KR) domain within the PKS module reduces the β-keto group to form the 3-OH-4-NH_2_ framework (Fig. 1c)^26^. A similar NRPS-PKS pair with a KR domain in the PKS module has also been observed in the BGCs of burkholdac^23^, hapalosin^28^, thalassospiramide^29^, and nosperin^21^. In contrast, the β-ketone functionality is retained in andrimid biosynthesis. Notably, the corresponding NRPS-PKS pair in the andrimid biosynthetic pathway lacks a KR domain, implying that the KR domain in PKS modules is responsible for 3-OH generation in Sta/Sta-like residue biosynthesis^30^. However, this pathway has not been experimentally verified and has only been rationalized based on the analysis of BGCs of natural products with the 3-OH-4-NH_2_ frameworks^26^.
In this work, we uncovered a unique post-assembly-line pathway for Sta biosynthesis that relies on a discrete oxidoreductase utilizing F_420_H_2_, a deazaflavin-based redox cofactor widely found in bacteria and archaea^31–33^. This pathway diverges from the conventional hypothesis, which attributes this function to a modular KR domain utilizing NADPH (Fig. 1c). Through gene knockout experiments and activation of the candidate pepstatin BGC, we characterized a noncanonical NRPS-PKS pathway responsible for pepstatin biosynthesis. Our findings suggest the involvement of in-trans and iterative NRPS and PKS mechanisms, indicating deviations from the traditional colinearity principle^34,35^. Deletion of pepI, encoding an F_420_H_2_-dependent oxidoreductase, resulted in an accumulation of the β-keto intermediates of pepstatins and related spontaneously decarboxylated products. Biochemical characterization of PepI in vitro unambiguously demonstrated the sequential reduction of β-ketones, starting with the central residue and then followed by the C-terminal moiety, ultimately leading to the formation of pepstatins. We determined the specific structural changes in the substrates and products of PepI through comprehensive structure elucidation and enzymatic characterization. The crystal structures of PepI and PepI in complex with the cofactor F_420_ allowed us to identify key residues His62, Tyr122, and Gln229. The roles of these residues are further rationalized by PepI-substrate modeling and site-directed mutagenesis studies. Moreover, biochemical assays utilizing a deuterium-labeled cofactor provide valuable insights into the catalytic mechanism of F_420_-dependent oxidoreductases. Notably, PepI-mediated Sta biosynthesis represents the only known iterative F_420_H_2_-dependent oxidoreductase, distinct from previously hypothesized PKS KR-dependent biosynthetic pathways for 3-OH-4-NH_2_ frameworks.
Results
Identification of the pepstatin BGC defying the colinearity rule
We cultivated the known pepstatin producer Streptomyces catenulae DSM40258^36^ and analyzed its fermentation broth using ultra-performance liquid chromatography-high-resolution mass spectrometry (UPLC-HRMS). Structural elucidation of the four purified pepstatin congeners (1-4) through nuclear magnetic resonance (NMR) spectroscopy revealed variations at the N-terminal acyl group, confirming congener 4 is a new derivative (Fig. 2a,b; Supplementary Figs. 1 and 26−42; and Supplementary Table 8)^10,11^.Fig. 2. Identification of pepstatins and the pep biosynthetic gene cluster.a UPLC-HRMS analysis (base peak chromatogram (BPC)) of pepstatin congeners (1-4) produced by Streptomyces catenulae DSM40258 (i); Knockingout pepD abolished pepstatin 1-4 production (ii); Pepstatin congeners (1-4) produced by heterologous expression of BGC pep in Del14 (Del14-pep) (iii); The production of 1-4 significantly decreased by pepJ deletion in Del14-pep-ΔpepJ (iv); The production of 1-4 increased in Del14-pep-pepJ-act by promoter exchange of pepJ (v). b The chemical structures of pepstatins isolated from Streptomyces catenulae DSM40258. c The schematic representation of the pepstatin BGC from S. catenulae DSM40258.
With pepstatin production verified, we performed complete genome sequencing of S. catenulae DSM40258 to decipher the BGC of pepstatin. Surprisingly, the absence of a straightforward candidate for an NRPS-PKS hybrid BGC suggested a noncanonical biosynthetic pathway. According to the colinearity principle, we expected to find five NRPS modules and two PKS modules in one BGC (Supplementary Fig. 2). However, none of the NRPS-related BGCs encoded more than four adenylation (A) domains, indicating an unconventional biosynthesis mechanism. Furthermore, we found no consecutive NRPS and PKS modules that matched the previously reported biosynthesis of statine/statine-like residues in the DSM40258 genome. Despite these unexpected challenges, we identified one NRPS-PKS hybrid BGC (designated as “pep”) with only three A domains that caught our attention. This BGC included one putative leucine-activating NRPS gene (pepB) adjacent to a PKS gene (pepC) with a truncated AT domain (Fig. 2c, Supplementary Table 5). To confirm the involvement of the pep BGC in pepstatin biosynthesis, we performed gene deletion of pepD, which encodes the potential alanine assembly module. Deleting the NRPS gene pepD completely abolished pepstatin production in S. catenulae DSM40258 (Fig. 2a; Supplementary Figs. 3 and 7a), demonstrating that pepD is essential for pepstatin biosynthesis.
To validate the biosynthetic pathway, the 18.3 kb pep BGC, comprising ten genes (pepA-J), was cloned and subsequently heterologously expressed in Streptomyces albus Del14^37^. The successful heterologous reconstitution of pepstatin production confirmed the BGC and its boundaries (Fig. 2a and Supplementary Fig. 4). Deletion of the LuxR-like transcriptional regulator gene pepJ significantly reduced pepstatin production, suggesting that pepJ functions as a positive regulator. Conversely, overexpression of pepJ under the kasOp promoter led to a more than 25-fold increase in pepstatin yield (Fig. 2a and Supplementary Figs. 5–7), enabling the identification of biosynthetic intermediates in subsequent studies.
A highly dissociated and nonlinear NRPS-PKS pathway for pepstatin biosynthesis
The streamlined pep BGC presents an interesting puzzle, as it contains fewer NRPS-PKS modules than the number of building blocks required for pepstatin biosynthesis, suggesting the involvement of noncanonical mechanisms. The pep BGC possesses only three A domains to assemble the pentapeptide backbone of pepstatins (Fig. 2c), which deviates from the colinearity principle. However, based on the chemical structure, pepstatin assembly hypothetically requires only three types of amino acids: a single l-alanine residue, and two occurrences each of l-valine and l-leucine (the precursor of statine), suggesting iterative use of A domains in its biosynthesis.
The A domain from the single-module NRPS gene pepD is predicted to activate alanine, while PepG, the stand-alone A domain protein, is predicted to activate threonine (Supplementary Table 5). PepH features an unusual C-PCP-C domain arrangement without any cognate A domains. PepG is likely promiscuous in substrate activation, capable of activating threonine and similar amino acids, including valine. However, the C domains in PepH might serve as gatekeepers, processing only proteins loaded with valine^38^. We propose that pepstatin biosynthesis initiates with the activation and in-trans loading of valine by PepG onto the PCP domain of PepH. The N-terminal C domain of PepH then acylates the Val-S-PepH species using various short-chain fatty acyl CoAs. A plausible subsequent step involves PepG reactivating valine and loading it onto the stand-alone PCP protein PepA. The C-terminal C domain of PepH may then facilitate chain extension by attacking the Val-S-PepA upon the thioester of the N-acyl-Val-S-PepH intermediate (Fig. 3).Fig. 3. Proposed pepstatin biosynthesis pathway.Fatty acids are likely activated to fatty acyl-CoA by acyl-CoA synthase and transferred to the carrier protein PepA, whereas PepG, PepH, PepB, PepC and PepD build up the peptide chain. The pentapeptide chain is subsequently released by PepE. Oxidation status changes are highlighted in turquoise to exhibit the two ketoreduction reactions catalyzed by PepI.
The A domain of the single-module NRPS gene pepB is predicted to activate leucine, while pepC, the sole PKS gene, encodes a KS-AT-ACP module. These findings suggest that PepB and PepC may collaborate to assemble the Sta residue backbone in pepstatins, similar to previously proposed Sta biosynthesis (Fig. 1c). However, the absence of a KR domain in PepB implies a remarkable new feature in Sta biosynthesis. We propose that PepB extends the nascent N-acyl-Val-Val chain with leucine, and PepC subsequently installs a malonyl-CoA to form the β-ketoacyl species. PepD then appears to activate and incorporate alanine into the growing NRP-PK chain. Following this, PepB and PepC may collaborate again to extend the lipopeptide backbone with a second β-ketoacyl building block. This second extension involving PepB and PepC following PepD, an unrelated NRPS module, is highly unusual and partially similar to the pass-back mechanism observed in thalassospiramide biosynthesis^39^. Notably, in pepstatin biosynthesis, this extension likely involves inter-protein interactions (Fig. 3), representing an in-trans mechanism distinct from intramodule interactions observed in other systems^39^. Overall, while the proposed pathway outlines a plausible biosynthetic logic, additional experimental data are needed to validate these hypotheses and clarify the unique enzymatic features of the pepstatin biosynthetic machinery.
The mechanism underlying the double reduction of the β-keto group during pepstatin biosynthesis remains unresolved due to the absence of a KR domain. The timing and nature of these unidentified reductions are particularly intriguing, given the presence of two Sta residues. We assumed it is likely that pepstatin biosynthesis, unlike other Sta-containing natural products, has evolved a unique β-keto reduction mechanism that may involve enzymes working either in tandem or sequentially. A prime candidate for this reduction process is PepI, a putative F_420_-dependent oxidoreductase, which shares low sequence identity (26.1%) with the TIM-barrel type F_420_-dependent methylenetetrahydromethanopterin reductase (Mer)^40^.
PepI is an F420H2-dependent ketone reductase
Deletion of the pepI gene in the heterologous expression system of the pep BGC abolished the production of 1-4, while a series of new peaks emerged, corresponding to unreduced β-keto intermediates 5-8 as identified by MS/MS analysis (Figs. 3 and 4a and Supplementary Figs. 8 and 9). However, the β-ketoacid compounds 5-8 decomposed rapidly through spontaneous decarboxylation into 9-12 (Fig. 4a), which lack the terminal carboxyl group, as confirmed by NMR analysis (Fig. 4d and Supplementary Figs. 10 and 43−62, Supplementary Table 9). Unlike the KR domain typically responsible for reduction during chain extension, the accumulation of the free β-keto intermediates (5-12) suggested that PepI functions as a tailoring enzyme, likely reducing the ketone groups at the β-position of the two β-diketone moieties after the intermediates are released from PepC (Fig. 3).Fig. 4. PepI catalyzes tandem ketone reductions.a UPLC-HRMS analysis of pepstatins and unreduced β-keto intermediates in the pepI deletion mutant. (i) EICs ([M + H]^+^, blue) of 1 (644.42), 2 (658.44), 3 (672.45), 4 (686.47) from the improved heterologous expression of pep (pepJact); (ii) EICs ([M + H]^+^, green) of 5 (640.39), 6 (654.40), 7 (668.42), 8 (682.44) and (iii) EICs ([M + H]^+^, purple) of 9 (596.40), 10 (610.42), 11 (624.44), 12 (638.45) from the pepI deletion mutant based on Del14-pep- pepJ-act. b Representative pep-like actinobacterial pathways classified into three types mainly distinguished by containing cis-AT PKS, trans-AT PKS, or without PKS. c In vitro characterization of kvPepI. EICs ([M + H]^+^, red) of 13 (598.42) and 17 (600.43) produced by kvPepI reaction with 9 and EIC ([M + H]^+^, orange) of 9 from the control reaction using boiled kvPepI and 9 were shown. d HSQC and HMBC slices of 9, 13, and 17, showing the structural changes at the Sta residue, decarboxylated Sta residue (DecSta), the precursor of Sta (PreSta), and the precursor of DecSta (DecPreSta). e Time-course of kvPepI using 9 as the substrate, supplemented with F_420, FGD, and G6P. BPCs of the reactions were shown.
To investigate this distinct mechanism of statine formation, we aimed to characterize PepI in vitro. Recombinant PepI was successfully purified from E. coli BL21 (DE3). However, the recombinant protein exhibited unsatisfactory solubility (Supplementary Fig. 11b), precluding its use in downstream structural biology studies. To address this challenge, we searched public databases for homologs of PepI and identified several pep-like BGCs harboring pepI gene homologs. These BGCs are classified into three distinct subtypes, primarily based on variations in their PKS genes (Fig. 4b, Supplementary Fig. 11a, and Supplementary Table 6). The pep BGC represents the first subtype, characterized by a cis-AT PKS gene, while the second subtype features a trans-AT PKS gene that lacks the AT domain. Notably, all PKS modules in these BGCs are devoid of KR domains. We therefore hypothesize that PepI analogs serve as substitutes for KR domains to generate the 3-OH-4-NH_2_ moiety. The third subtype, however, lacks homologs of PepC and PepD, raising questions about its ability to produce Sta/Sta-like residues containing products (Fig. 4b). Among these, the homolog kvPepI from Kitasatospora viridis DSM44826, with 53.3% sequence identity to PepI, was more amenable to study (Supplementary Fig. 11b). Searching pepI homologous genes in genomes of producers of didemnin^27^, burkholdac^23^, hapalosin^28^, thalassospiramide^29^, and nosperin^21^ did not lead to any hit, further corroborating the unique Sta formation in pepstatin pathway.
We reasoned that 5-8 are likely the authentic intermediates for 1-4, but only the decarboxylated products 9-12 were stable enough to be isolated in sufficient quantities for in vitro assays. We primarily used the most abundant congener, 9, as the substrate in all PepI and kvPepI assays. To provide and regenerate the reduced cofactor F_420_H_2_, we supplemented the reaction mixture with F_420_, the F_420_-dependent glucose-6-phosphate dehydrogenase (FGD)^41^, and its substrate glucose-6-phosphate (G6P). After overnight incubation with PepI or kvPepI, UPLC-HRMS analysis revealed the complete consumption of 9 and the appearance of a new single-charged ion with a 4 Da increase, indicating the reduction of two ketones in 9 (Fig. 4c, Supplementary Figs. 10 and 12−14). Subsequently, we scaled up the kvPepI enzymatic assay using 9, which allowed us to purify new product 17 for NMR analysis, confirming the presence of the middle β-hydroxyl group and C-terminal secondary alcohol (Fig. 4d, Supplementary Figs. 68−72 and Supplementary Table 10).
We observed the same 4 Da mass shift using 10, 11, or 12 as substrates for PepI or kvPepI, indicating consistent dual ketone reduction supported by MS/MS analysis (Supplementary Figs. 10 and 12−14). Since the authentic substrates 5-8 were too unstable for isolation due to the rapid spontaneous β-keto decarboxylation, we used the fermentation broth of the mutant Del14-ΔpepI for in vitro assays. As anticipated, the incubation with PepI resulted in the production of 1-4, as detected by UPLC-HRMS (Supplementary Fig. 15). These results confirmed that PepI is the enzyme responsible for the dual ketone reduction in pepstatin biosynthesis. Removing F_420_, FGD, or G6P abolished PepI or kvPepI activity, underscoring the essential role of F_420_H_2_ in these transformations (Supplementary Figs. 13 and 14).
PepI catalyzes the tandem reduction of two ketones
With the role of PepI in reducing ketones during pepstatin biosynthesis confirmed, we focused on the timing of the two reduction steps. During our investigation, in addition to product 17, we identified a previously uncharacterized intermediate, 13, which was only 2 Da heavier than 9 (Fig. 4c). This led us to hypothesize that 13 could be an intermediate of 9 with only one of the ketones reduced. MS/MS and NMR analysis unambiguously determined the structure of purified 13. The HSQC and HMBC correlations of 13 clearly indicated the presence of a β-hydroxyl group at the middle residue (Sta3), with the methyl ketone at the terminal position remaining unchanged (Fig. 4d, Supplementary Figs. 10, 16, 58−62 and Supplementary Table 10). These findings are also corroborated by MS/MS analysis of the corresponding intermediates with an additional 2 Da when using 10, 11, or 12 as substrates (Supplementary Figs. 10 and 16).
To further examine the order of the two ketone reductions, we conducted time-course experiments using kvPepI. The time course-assay of kvPepI showed that 13 appeared first and reached the maximum concentration within three hours. Compound 17 emerged later than 13 and became apparent after one hour of incubation. The amount of 17 kept increasing for 5 h until 9 and 13 were nearly consumed completely (Fig. 4e). These results indicate that the reduction of the middle β-ketoamide moiety occurs before the reduction of the terminal ketone, establishing the sequential nature of PepI’s catalytic activity.
Structure of kvPepI
To better understand the mechanism underlying the reduction reaction, we determined the crystal structures of kvPepI and its complex with the cofactor F_420_, both to a resolution of 1.65 Å (Supplemtary Table 7). We found that kvPepI is structurally similar to other members of Class I F_420_-dependent enzymes (Fig. 5a, Supplementary Fig. 19a, b), including F_420_-dependent alcohol dehydrogenase (Adf, PDB ID: 1RHC; Supplementary Fig. 19c, C \documentclass[12pt]{minimal} \usepackage{amsmath} \usepackage{wasysym} \usepackage{amsfonts} \usepackage{amssymb} \usepackage{amsbsy} \usepackage{mathrsfs} \usepackage{upgreek} \setlength{\oddsidemargin}{-69pt} \begin{document}$$\alpha$$\end{document} RMSD over entire length of the protein: 2.9 Å)^42^. Upon F_420_ binding, the kvPepI structure remains virtually unchanged, except for the stabilization of the residues 187–190 (Fig. 5a and Supplementary Fig. 20) that are part of a larger flexible loop (residues 181–201). This loop forms a lid over the lactyloligoglutamyl tail of F_420_, likely anchoring the F_420_ for catalysis. A number of hydrogen bonds and hydrophobic interactions further stabilize the cofactor (Supplementary Fig. 21a). Interestingly, the C5 of F_420_ was found to be positioned within 3.8 Å of a water molecule, held in place by His62 and Tyr122 (HOH570; Supplementary Fig. 21b). Overlay of Adf-acetone adduct structure with kvPepI-F_420_ revealed that the keto group of the acetone adduct occupies a position similar to that of the ordered water (HOH570, Fig. 5b, Supplementary Fig. 21a), suggesting that the highly conserved His62 acts as a general acid to protonate the keto group of 9. The His imidazole moiety likely acts as a proton relay through substrate protonation via the His62-Nɛ2 position and interaction with the carboxyl group of the Glu126 sidechain via the His62-Nδ1 (Supplementary Fig. 21b). Accordingly, the H62A mutation abolished the PepI activity (Fig. 5d, e). To rule out the possibility of H62A mutation causing a loss of activity due to allosteric effects, we also solved the structures of kvPepI^H62A^ and kvPepI^H62A^ in complex with F_420_, which are virtually identical to kvPepI apo and kvPepI-F_420_ complex structures, respectively (Supplementary Fig. 21c and Supplementary Table 7). Taken together, these findings strongly support the role of His62 as the proton-donating residue.Fig. 5. Structural analysis, molecular modeling, and biochemical assays of kvPepI and mutants.a Superposition of the kvPepI structure with (gray) and without (slate) F_420_ bound. Changes in the overall structure of the protein are minimal (Cα RMSD of 0.15 Å over all non-hydrogen atoms), except for the stabilization of a loop (residues 187 – 190; yellow line) that serves as a lid over the bound cofactor. b Hypothetical binding pose of U-shaped 9 in kvPepI – F_420_ complex structure. The missing loop (pink) was modeled using AlphaFold^68,69^. The orientation and conformation of 9 were modeled based on experimental data regarding the position of hydride transfer, as well as loss-of-activity-conferring amino acid mutations (details see experimental section). F_420_ (orange) and 9 (pale green) are shown as sticks (atom color: carbon black, nitrogen blue, oxygen red). c Schematic 3D representation of kvPepI – F_420_ interactions with modeled pose of 9. Hydrogen bonds are depicted with dotted yellow lines with distances given in Å, while all other residues form hydrophobic interactions with the substrate. The residues are colored according to the conservation score calculated using the ConSurf server^74,75^. Reactions using 9 (d) or 13 (e) as the substrate with kvPepI (i), Q289A (ii), Y122F (iii), Q229A (iv), Y122A (v), H62A (vi), and boiled kvPepI as negative control (vii). BPCs of reactions were shown.
Substrate mode of binding and mutational analysis of kvPepI
Despite repeated attempts, we could not determine the structure of either kvPepI or kvPepI-F_420_ in complex with 9. Therefore, we decided to model 9 in the kvPepI-F_420_ crystal structure using the gathered experimental data as well as the above-mentioned ordered water molecule to guide the position of the β-keto group of the oxidized statin precursor residue PreSta3 residue in 9 (Fig. 5b, c). For 9 two different binding modes were considered: linear and U-shaped conformation (Supplementary Fig. 22). However, only in the U-shaped conformation are two relatively well-conserved residues, Gln229 and Gln289, located close to the terminal end of the U-shaped 9 in the binding pocket (Fig. 5c and Supplementary Fig. 23c), forming hydrogen interactions with the amide bond of Val1 of 9. We reasoned that if these residues are critical for binding of 9, mutations to Ala should impair activity. Both Gln289A and Gln229A mutations were found to either result in complete loss of activity or impaired turnover of 9 and/or 13 (Fig. 5d, e). These data strongly support the binding of 9 in a U-shaped conformation. Moreover, a U-shaped conformation of 9 also nicely places the hydrophobic sidechains of 9 into hydrophobic pocket of the enzyme (Fig. 5b and Supplementary Fig. 23a) comprising residues that show varying degree of conservation (Fig. 5c, Supplementary Fig. 23b). Compound 9 is held in place primarily by hydrophic interactions such that it positions the carbonyl group (point of hydride attack) towards the F_420_ and His62 to ensure the correct enantioselective outcome of the reaction (Fig. 5c and Supplementary Fig. 25; vide infra).
The ketone is optimally placed for proton/hydride transfer, with the carbonyl carbon placed 2.9 Å and 3.8 Å from the Nɛ of His62 and C5 of F_420_, respectively. The side chain of Tyr122 packs against the Leu side chain and the β-keto group of PreSta3 of 9 (2.7 Å; Fig. 5c and Supplementary Fig. 23c). We thus wondered whether Tyr122 played a role in ketone reduction and produced kvPepI^Y122A^ and kvPepI^Y122F^. When we tested the effect of kvPepI^Y122A^ on 9, we found ketone reduction to be significantly impaired, with only trace amounts of 13 observed (Fig. 5d). In contrast, kvPepI^Y122F^ resulted in an accumulation of 13 (Fig. 5d). Moreover, we tested the activities of kvPepI^Y122A^ and kvPepI^Y122F^ in comparison to kvPepI using purified 13 and observed only a tiny amount of 17 with kvPepI^Y122F^ but no formation of 17 was observed with kvPepI^Y122A^ (Fig. 5e). This implies that Tyr122 is crucial and acts at two points during catalysis: a) binding of 9, with hydrophobic interaction between phenyl ring and Sta helping orient the substrate for catalysis (Fig. 5c and Supplementary Fig. 23a, c), and b) during the second round of reduction by forming hydrogen bonding with 13. This likely involves the reduced ketone as kvPepI^Y122F^ and kvPepI^Y122A^ compared to kvPepI, either resulting in complete or significant loss of activity upon incubation with 13 (Fig. 5e). A comparison of the structure of kvPepI^Y122A^-F_420_ complex to the corresponding structure of the wild-type holoenzyme revealed no major structural perturbations caused by the mutation (Supplementary Fig. 23d and Supplementary Table 7).
Whether the kvPeI employs either processive^43^ or distributive catalysis^44^ is not clear. The accumulation of 13 during time-course experiments (Fig. 4e) hints towards the latter. The conformational changes required to position the second keto reduction site close to His62 could be facilitated by the flexible loop located above the Sta (Fig. 5b; magenta). The first ketone reduction may also allow the formation of intra- and intermolecular hydrogen bonding, assisting reorientation of 13. Therefore, we envision a scenario where all the aforementioned factors likely contribute to the conformational change(s) needed to position the second keto group close enough to His62 for hydride transfer. Despite persistent efforts, we encountered challenges in obtaining the structure of kvPepI or variants in complex with F_420_, 13 or 17. Therefore, further studies are needed to gain a deeper understanding of the binding mode and molecular mechanism of the second keto reduction.
Hydride transfer from F420H2 to the keto carbon
Since we observe only the S-enantiomer of 9, the specific orientation of substrate towards the F_420_ and His62 must be decisive in the enantioselective outcome of the reaction. To shed light on how and where the hydride is transferred from the C5 atom of F_420_H_2_, we performed kvPepI assays with deuterium-labeled reduced F_420_-5-d_1_. This labeled cofactor was synthesized through a coupled reaction using d-Glucose-1-d_1_ and hexokinase. Intermediates 13 and 17 were successfully produced and the main mass isotope ion increased by 1 and 2 Da, respectively (Fig. 6a). The mass shift indicates the incorporation of one deuterium in 13 and two deuteriums in 17. To determine the exact position of incorporation, we purified the labeled 13 and 17 from a scaled-up reaction. The NMR analysis unambiguously confirmed that the deuterium is attached to the carbon atom bearing the hydroxyl group (reduced from the ketone) (Fig. 6b, Supplementary Figs. 73−74 and Supplementary Table 10). These findings demonstrate that a direct hydride shift takes place from the cofactor to the carbonyl carbon. Furthermore, the stereo-configuration (S) of the carbon attached to the hydroxyl group in the middle Sta residue provides insight into the orientation of the pepstatin peptide backbone within the active site. In order to achieve the observed S-configuration while enabling protonation from His62 (vide supra), the peptide chain needs to be oriented as shown in Figs. 5c and 6c.Fig. 6. Deuterium-labeled assays and mechanistic considerations for PepI.a MS analysis of 13 and 17 in the kvPepI and 9 reactions without (i: 13, iii: 17, blue) or with (ii: 13-d1, iv: 17-d2, red) F_420_-5-d_1_ provided by the coupled hexokinase assay using d-Glucose-1-d_1_. b The 2 Da increase in the molecular mass indicated 17-d2 was the deuterated derivative of 17. The position of deuteration was deduced by comparing the ^1^H-NMR spectra.The methyl group H1-DecSta5 in 17-d2 showed a singlet whereas in 17 it was a doublet, together with the disappearance of the H2-DecSta5 signal in 17-d2, indicating the H2-DecSta5 was deuterated. Similarly, the H3-Sta3 was deuterated, as evidenced by the disappearance of H3-Sta3 signal and splitting pattern change of H2-Sta3. c Proposed reaction mechanism derived from the experimental observations indicates the orientation of the pepstatin peptide backbone in relation to His62 and F_420_ to achieve the observed S-product. R represents the lactyloligoglutamate tail of F_420_.
Discussion
Pepstatins have gained significant attention due to their potent inhibitory effects against various APs, which are promising therapeutic targets for treating a number of important diseases^7^. Despite this interest, the biosynthesis pathway of pepstatins has remained unknown. In this study, we identified the NRPS-PKS hybrid BGC responsible for pepstatin biosynthesis and revealed its distinctive disconnected and iterative utilization pattern. Most notably, we uncovered a unique F_420_H_2_-dependent post-assembly modification mechanism, which plays a crucial role in constructing the essential 3-OH-4-NH_2_ framework. This mechanism differs significantly from the previously hypothesized PKS KR-dependent pathway observed in the biosynthesis of other natural products (Fig. 1c)^26^.
The concise pepstatin assembly line stands out due to its highly disconnected nature, featuring unusual trans-acting and iterative enzymes. The potential iterative use of the discrete A domain PepG and its in-trans cooperation with PepH and PepA warrant further in-depth investigation into the biosynthetic mechanism. Furthermore, the stand-alone NRPS/PKS modules (PepB, PepC, and PepD) involved in the assembly of the Sta-Ala-Sta chain may operate through mechanisms distinct from those proposed for thalassospiramide biosynthesis, which involves a cross-modular pass-back chain extension strategy within a single multimodular megaenzyme^39^.
F_420_-dependent oxidoreductases have been reported in several natural product biosyntheses, typically mediating the hydrogenation of different double bonds in alkene, ketone, and imine moieties^45–53^. Notably, PepI stands out as the only biochemically characterized F_420_-dependent oxidoreductase capable of performing two rounds of reductions, underscoring the iterative fashion of pepstatin biosynthesis. Deletion of pepI led to the accumulation of β-diketone intermediates and the loss of pepstatin production. Through comprehensive structural and biochemical characterization of PepI/kvPepI, we confirmed that PepI/kvPepI sequentially reduces the middle β-ketone followed by the C-terminal β-ketone or methyl ketone.
Site-directed mutagenesis and kvPepI-9 modeling studies support the role of His62 as a potential catalytic residue, as corroborated by the abolishment of enzymatic activity regardless of whether 9 or 13 were used as the substrate. Two additional residues, Tyr122 and Gln229, were also found to be critical for PepI activity and, based on the modeling studies, are likely to be involved in substrate binding. Interestingly, mutating Tyr122 to Phe had a much greater effect on the second ketone reduction compared to the first step reduction, suggesting the vital role of the hydroxyl group of Tyr122 in positioning the substrate for the second reduction. In addition, the loss of kvPepI activity in the Q229A mutant supports the crucial role of Gln229 in stabilizing the substrate binding by forming hydrogen bonding in the modeling prediction. Interestingly, structural tolerance of the C-terminal ketone reduction indicates that the diketone is not a prerequisite for PepI activity. Further studies are currently underway to understand how 13 is oriented within the active site during the second reduction step.
In conclusion, this study unveils the long-sought-for, highly dissociated, and iterative biosynthetic pathway of pepstatins. The discovery of the KR domain-independent 3-OH-4-NH_2_ framework biosynthesis and the characterization of PepI as a tandem F_420_H_2_-dependent oxidoreductase expand the NRPS/PKS biosynthetic repertoire. Moreover, the data presented here on the PepI mechanism will likely contribute to a better understanding of underinvestigated F_420_-dependent oxidoreductases.
Methods
Bacterial strains, plasmids, and DNA manipulation
Bacterial strains and plasmids used in this study are listed in Supplementary Tables 1 and 2, respectively. All primers used in this study (listed in Supplementary Table 3) were synthesized by Sigma-Aldrich (Steinheim, Germany). In-silico analyses, including primers design, BGC annotation, and short-read mapping, were conducted using Geneious Prime® 2022.2.2 (Biomatters Ltd., New Zealand). E. coli DH10B was employed for general subcloning purposes. Plasmid DNA isolation kits were obtained from Qiagen. Q5® High-Fidelity DNA polymerase and HiFi DNA Assembly Mater Mix were procured from New England Biolabs (Ipswich, MA). Restriction enzymes and other standard molecular biology reagents were purchased from Thermo Scientific. All kits and enzymes were used in accordance with the manufacturers’ protocols. Red/ET recombineering–based plasmid modifications were performed using E. coli GB08-red, as described in previous studies^54,55^. Genomic DNA of Streptomyces strains was manually extracted following a cetyltrimethylammonium bromide-based protocol^56^.
Strain cultivation
E. coli was cultivated in LB medium (10 g/L tryptone, 5 g/L NaCl, 5 g/L yeast extract, pH 7.6) at 37 °C with shaking at 180 rpm. All Streptomyces strains were cultivated at 30 °C with shaking at 200 rpm. For Streptomyces catenulae DSM40258 and heterologous expression mutants, cells were grown in tryptone soya broth (TSB) medium (30 g/L TSB) for genomic DNA isolation, conjugation, or as starter cultures prior to fermentation. Conjugations were performed on MS agar plates (d-mannitol 20 g/L, soya bean meal 20 g/L, agar 20 g/L). Streptomyces catenulae medium (30 g/L glucose, 20 g/L corn steep liquor, 0.5 g/L dipotassium hydrogen phosphate, 0.2 g/L ammonium sulfate, 0.5 g/L magnesium sulfate, 5 g/L calcium carbonate, pH 7.0)^57^ was used for fermentation. Fermentation cultures were inoculated from 3 to 4 days TSB starting cultures (10% (v/v) inoculation volume) and cultivated for 4 days (24 h for Del14-pep-ΔpepI).
Genome sequencing and analysis
The genome of Streptomyces catenulae was sequenced using Illumina HiSeq and MinION Nanopore sequencing technologies at the genome analytics facility of the Helmholtz Centre for Infection Research (Braunschweig, Germany). BGCs were predicted by antiSMASH (http://antismash.secondarymetabolites.org/)^58^.
Construction of gene pepD deletion plasmid
The pepD gene in the chromosome of Streptomyces catenulae was deleted using the CRISPR-Cas9 gene editing tool pQS9, following previously described methods^59^. Spacer inserts, which included a gene-specific 20-nt guide sequence, were generated by annealing two 34-nt synthesized oligonucleotides, sgpepD-f and sgpepD-r. The annealed oligonucleotides were cloned into pQS9 at NcoI-XbaI to afford psgQS9-ΔpepD and verified by Sanger sequencing. The flanking region of gene pepD, 2 kb on each side, served as homologous recombination repair templates following Cas9-mediated gene editing. The 2.0 kb upstream homologous arm (UHA) and 2.0 kb downstream homologous arm (DHA) were amplified from genomic DNA of Streptomyces catenulae using primer pairs pepD-L-f/pepD-L-r and pepD-R-f/ pepD-R-r, respectively. These amplified fragments were cloned into psgQS9-ΔpepD at StuI using the Gibson assembly cloning kit, resulting in the plasmid pQS9-ΔpepD, which was verified by SalI digestion.
Heterologous expression of the pep BGC
The potential pepstatin BGC pep was divided into three fragments, each ~6 kb in size, with 20 bp homologous arms flanking both ends. These fragments were amplified using the primer pairs pep-1-f/pep-1-r, pep-2-f/pep-2-r, and pep-3-f/pep-3-r, respectively. Concurrently, the backbone plasmid was amplified using the primer pair p15A-f/p15A-r. The amplified plasmid backbone and the three pep gene cluster fragments were assembled via Gibson assembly, resulting in the formation of the plasmid p15A-pep.
Subsequently, a 4.3 kb phi31 integrase-apramycin resistance gene cassette was excised from the pR6K-phiC31-oriT plasmid through AseI digestion. This cassette was then introduced into the p15A-pep plasmid via Red/ET recombineering, yielding the recombinant plasmid p15A-int-pep. Plasmid p15A-int-pep was verified by NcoI digestion.
Pathway engineering of the pep BGC for heterologous expression
The gene pepJ in p15A-int-pep was replaced by the chloramphenicol resistance gene (cml), which was amplified using the primers pepJ-ko-f and pepJ-ko-r, via Red/ET recombination^2,54^. This process yielded the plasmid p15A-int-pep-ΔpepJ.
To enhance pepstatin production in the heterologous expression mutant, the upstream non-coding region of gene pepJ in plasmid p15A-int-pep was substituted with a cml-kasO cassette using Red/ET recombination, resulting in the plasmid p15A-int-pep-kasop-pepJ^55^.
For pepI inactivation, both pepI and the upstream non-coding region of pepJ in plasmid p15A-int-pep were replaced with cml-kasO cassette via Red/ET recombination, producing the plasmid p15A-int-pep-ΔpepI^55^.
Conjugation
In this study, we employed an adapted biparental or triparental conjugation protocol^56^ to introduce exogenous DNA into S. catenulae or S. albus Del14, respectively. The donor strain used for biparental conjugation was E. coli ET12567/pUZ8002. For triparental conjugation, the donor strain was E. coli DH10B, with E. coli HB101/pRK2013 serving as the helper strain.
After conjugation, the plates were allowed to dry and then further incubated at 30 °C until the exconjugants became visible, typically within 3−5 days. Visible exconjugants were inoculated to TSB media for genome DNA isolation. Each exconjugant was verified by PCR amplification with relevant primers (Supplementary Table 3).
Gene cloning and protein purification
The codon-optimized pepI gene was synthesized by GenScript and subsequently amplified using the primers pepI-f/pepI-r. The amplified pepI was cloned into the plasmid pCold I, resulting in the plasmid pCold-pepI. Additionally, the plasmids pET28b-sfpepI, pET28b-svpepI, and pET28b-kvpepI were ordered from GenScript.
For expressing the kvPepI site-directed mutants, H62A, Y122F, Y122A, and Q229A, plasmid pET28b was digested with NdeI/HindIII for cloning. The kvpepI gene was split into two parts, and the specific mutations were introduced at the junction through primers listed in Supplementary Table 3. The resulting mutant fragments were assembled into the plasmid pET28b via Gibson assembly. For the Q289A mutant, the pET28b plasmid was amplified using the primer pair pET-28b-f/pET-28b-r to serve as the backbone. The mutation was introduced through primers (listed in Supplementary Table 3) at the junction and cloned to plasmid pET28b by Gibson assembly.
All expression constructs were transformed into BL21 (DE3) cells. For protein purification, cells were grown overnight in LB containing relevant selection pressure at 37 °C. This overnight culture was diluted 1:100 into fresh LB medium supplemented with the appropriate antibiotics and incubated at 37 °C with shaking for 3−4 h. Until optical density (OD_600_) reached 0.6, the culture was rapidly cooled to 16 °C in ice water for 30 min. Subsequently, isopropyl β-d-1-thiogalactopyranoside (IPTG) was added to a final concentration of 0.1 mM to induce protein expression. The culture was then incubated with shaking at 16 °C for 16 h. Following this incubation period, the cells were harvested by centrifugation.
For protein purification, cell pellets were resuspended in lysis buffer (20 mM Tris pH 8.0, 200 mM NaCl, 10% glycerol (w/v), 20 mM imidazole, 1 mM TCEP) supplemented with cOmplete EDTA-free protease inhibitor tablets (Roche). The cell suspension was lysed by two passages through a cell disrupter (30 kpsi, Microfluidics Corp.), and the cell debris was removed by centrifugation at 40,000 × g for 30 min at 4 °C. The supernatant was then loaded onto a 5 mL HisTrap HP column (GE Healthcare) pre-equilibrated with the lysis buffer. The column was washed with 30 column volumes of lysis buffer, and the bound protein was eluted using an elution buffer (lysis buffer with 250 mM imidazole).
Fractions containing the target protein were subjected to size-exclusion chromatography using a HiLoad 16/600 Superdex 200 pg column (GE Healthcare) pre-equilibrated with gel filtration buffer (50 mM Tris pH 8.0, 200 mM NaCl, 1 mM TCEP). Protein purity was assessed by SDS-PAGE, and the fractions containing the highest purity protein were pooled and concentrated to approximately 5 mg/mL. The protein concentration was determined using a Nanodrop UV-Vis spectrophotometer at 280 nm, with theoretical extinction coefficients calculated using the ExPASy ProtParam tool.
Enzyme assay conditions
The crude extract containing compounds 5-8 previously stored at −80 °C, was dissolved in pre-cooled methanol to a concentration of 1 mg/mL and stored on ice. Purified compounds 9-12 were separately dissolved in methanol to create 1 mM stock solutions. The F_420_ and FGD enzyme used in the activity assays were prepared as previously described^60,61^.
A 50 µL reaction mixture was prepared in 1.5 mL Eppendorf tubes, containing 0.6 µM PepI, kvPepI, or other mutants, 20 mM Tris-HCl (pH 7.5), 10 µM F_420_, 2.5 mM glucose 6-phosphate, 0.45 µM F_420_-dependent glucose-6-phosphate dehydrogenase (FGD) and 10 µM substrate (or 2 µg crude extract). In the time-course experiments of kvPepI, substrate concentration was reduced to 1 µM. Unless otherwise noted, the reaction mixture was incubated at 30 °C for 5 h, then quenched with 0.2 M HCl, and stored at −80 °C until ready for analysis.
Before LC-MS analysis, an equal volume of methanol was added to the reaction mixture, and it was centrifuged at 8000 × g for 15 min at 15 °C to remove all the particles.
Sample preparation and UPLC-ESI-MS analysis
For small-scale fermentation (50 mL), Streptomyces cultures were harvested by centrifugation at 8000 × g for 15 min at 15 °C. The supernatant was supplemented with 2% (v/v) XAD16N resin and stirred for 2 h, followed by extraction with 50 mL methanol. The pelleted cells were resuspended in 50 mL methanol and agitated for 2 h. All fractions were evaporated to dryness under vacuum and then dissolved in 1 mL methanol to produce the crude extracts. The crude extract (10 μL) was diluted fivefold to 50 μL and centrifuged at 21,500 g for 15 min at 15 °C before UPLC-MS analysis.
Reverse phase UPLC-MS analysis was carried out using the following system and method. LC: Ultimate 3000 RS; HRMS: Bruker Maxis II (4Generation) Q-TOF using the Apollo II ESI source.; MS: Bruker amaZon speed ion trap mass spectrometer; Column: ACQUITY UPLC BEH C18 Column, 130 Å, 1.7 µm, 2.1 mm × 50 mm (Waters); Eluents: A: distilled water supplemented with 0.1% formic acid and B: distilled acetonitrile supplemented with 0.1% formic acid; Flow rate: 0.6 mL/min; column temperature: 45 °C. The gradient was as follows: (1) a 0.5 min isocratic step at 5% B, changed from 5% to 95 % B in 9 min, maintained at 95 % B for 1 min, decreased to 5% B in 0.5 min, and sustained 5% B for 2 min. (2) a 0.5 min isocratic step at 5% B, followed by a linear increase to 95% B in 18 min, maintained at 95 % B for 2 min, then equilibrated to the starting conditions (5% B) for 2 min. The UV-Vis spectra were recorded by a diode array detection (DAD) in the range from 200 to 600 nm. The mass detection was performed in the positive ESI mode. All HPLC-MS data were analyzed by Compass Data Analysis version 4.4 (Bruker Daltonics).
Compounds purification
To purify compounds 1-4, the cells and XAD16N resin from a 3-liter S. catenulae culture were harvested by centrifugation. The combined cells and resin were extracted with methanol. The extracts were concentrated using a rotary evaporator and then partitioned between methanol and hexane. The methanol phase was dried and further purified on a Sephadex LH-20 column (GE Healthcare) with methanol as the mobile phase. Fractions were pooled based on HPLC-MS analysis and were further purified by HPLC.
Semi-preparative purification of pepstatins was performed on an HCT HPLC-MS system using a Waters XSelect Peptide CSH C18 column (5 μm, 10 × 250 mm). The HPLC conditions were as follows: solvent A, H_2_O ( + 0.1% formic acid), and solvent B, ACN ( + 0.1% formic acid), at a flow rate of 5 mL/min and a column thermostatic at 45 °C. The gradient starts with a 2-minute isocratic step at 25 %B, followed by a ramp to 53%B in 16 min, maintained at 95%B for 3 min before returning to the initial condition in 2 min and re-equilibration for 2 min.
To purify compounds 9-12, a 3-liter culture of S. albus Del14-pep-ΔpepI was grown in liquid medium for 2 days, followed by the addition of activated carbon (1%, w/v). After centrifugation, the supernatant was removed, and the cells with activated carbon were extracted with methanol. The extracts were dried, and partitioned between ethyl acetate and deionized water (1:1, v/v). The organic phase containing compounds 9-12 was concentrated by rotary evaporation, and subsequently fractionated using flash chromatography on a Biotage Isolera One system with a 25 g Snapfit column. Elution was performed with ethyl acetate and methanol in the following gradient: 5 CV (column volume) of ethyl acetate, followed by a 10 CV linear increase from 0 to 20% methanol, and then a 10 CV linear increase from 20 to 100% methanol. Fractions were collected and further purified using a Dionex Ultimate 3000 SDLC low-pressure gradient system with a Waters XSelect Peptide CSH C18 column (5 μm, 10 × 250 mm). The gradient conditions were as follows: 0−2 min, 20%B; 2−12 min, 20−50%B; 12−15 min, 50-56%B; 15−17 min, 56−95%B; 17−19 min, 95%B; 19−-21 min, 95-20%B; 21−23 min, 20%B, with H_2_O ( + 0.1% formic acid) as eluent A and ACN ( + 0.1% formic acid) as eluent B. The separation was carried out with a column temperature of 45 °C at a flow rate of 5 mL/min.
To purify compounds 13 and 17, an in vitro ketoreduction reaction of substrate 9 was performed using the enzyme kvPepI, scaled up proportionally to 600 µL according to the method described in enzyme assay conditions. The reactions were quenched and extracted with ethyl acetate. The extracts were then concentrated and purified by HPLC, using the same separation conditions as those for intermediates 9-12.
Statine residue conformation verification
For l-statine (AAT Bioquest): Prepare two 1.5 ml Eppendorf tubes and add 50 µl of 10 mM l-statine solution to each. Adjust pH to approximately 9 by adding 20 µl of 1 M NaHCO_3_ to each tube. Then, add 20 µl of 1% Marfey’s reagent^62^ in acetone (d-FDLA and l-FDLA, respectively) to each tube, and incubate at 40 °C with shaking at 700 rpm for 1 to 2 h. Subsequently, neutralize the reaction by adding 10 µl of 2 N HCl, then dilute with 300 µl of acetonitrile. Centrifuge the mixture at 8000 × g for 15 min at 15 °C before UPLC-MS measurement. An aliquot (1 µL) of the analyte was injected, and the separation was achieved on a Waters Acquity BEH C18, 100 × 2.1 mm, 1.7 µm column using H_2_O ( + 0.1 % FA) and ACN ( + 0.1 % FA) as eluents. The flow rate is 550 µL/min at a column temperature of 45 °C.
For compounds 9, 13, 17, and 1, samples (approximately 100 µg each) were placed in 1.4 ml glass vials and heated in 100 µl of 6 M HCl at 110 °C for 45 min. The solvent was evaporated using a nitrogen flow at room temperature, and the residues were dissolved in 110 µL of H_2_O. Derivatization and analysis were performed in the same way as described above.
NMR conditions
NMR data were recorded in methanol-d4 or DMSO-d6 on a 500 MHz Avance III (UltraShield) spectrometer or a 700 MHz Avance III (Ascend) spectrometer, each equipped with a Helium-cooled CryoProbe (TCI). All observed chemical shift values (δ) are given in ppm and coupling constant values (J) in Hz. Chemical shifts were calibrated internally to the residual signal of either methanol-d4 (δH 3.31, δC 49.1) or DMSO-d6 (δH 2.50, δC 39.5). Multiplicities are described using the following abbreviations: s = singlet, d = doublet, t = triplet, q = quartet, dd = doublet of doublets, m = multiplet, br = broad signal.
Compound characterization
Acetyl-pepstatin (1): the molecular formula of 1 was determined to be C_31_H_57_N_5_O_9_ by High-resolution ESI-MS, m/z 644.4230 [M + H]^+^ (calcd. for C_31_H_58_N_5_O_9_, 644.4229). Analysis of the 1D and 2D NMR spectra (Supplementary Figs. 26−29, Supplementary Table 8), as well as the MS/MS fragmentation pattern (Supplementary Fig. 1), revealed that 1 has a peptide sequence of Ac-Val-Val-Sta-Ala-Sta. Hence, 1 was determined to be acetyl-pepstatin.
Propionyl-pepstatin (2) had the molecular formula C_32_H_59_N_5_O_9_, m/z 658.4383 [M + H]^+^ (calcd. for C_31_H_60_N_5_O_9_, 658.4386). The 1D NMR spectra of 2 were almost identical to that of 1, except for an additional CH_2_ group. Further interpretation of the 2D NMR data revealed a propionylated N-terminus. Thus, 2 was identified as propionyl-pepstatin (Supplementary Figs. 30−33, Supplementary Table 8).
Isobutyryl-pepstatin (Pepsinostreptin A) (3) had the molecular formula C_33_H_61_N_5_O_9_, m/z 672.4518 [M + H]^+^ (calcd. for C_33_H_62_N_5_O_9_, 672.4542). The 1D and 2D NMR spectra of 3 were similar to that of 1, the only difference was the N-terminal isobutyl group instead of the singlet methyl group. The structure of 3 was determined as isobutyryl-pepstatin (Supplementary Figs. 34−38, Supplementary Table 8).
2-methylbutanoyl-pepstatin (4) had the molecular formula C_34_H_63_N_5_O_9_, m/z 686.4660 [M + H]^+^ (calcd. for C_34_H_64_N_5_O_9_, 686.4699). The NMR data (Supplementary Figs. 39−42, Supplementary Table 8) and MS/MS fragmentation data (Supplementary Fig. 1) showed that 4 has the same amino acid sequence as 1-3. Thorough examination of the NMR data revealed that the fatty acid chain of 4 consisted of one methine group (δH-2 2.36, δC-2 43.4), one methylene group (δH-3 1.38/1.61, δC-3 28.3), and two methyl groups (δH-4 0.87, δC-4 12.4; δH-5 1.11, δC-5 18.2), indicating a 2-methylbutyl moiety. Therefore, the structure of 4 was characterized as 2-methylbutanoyl-pepstatin.
The molecular formula of compound 9 was determined to be C_30_H_53_N_5_O_7_ by ESI-HRMS, m/z 596.4017 [M + H]^+^ (calcd. for C_30_H_54_N_5_O_7_, 596.4018). 1D and 2D NMR data (Supplementary Figs. 43−47, Supplementary Table 9) in combination with mass spectrometric analysis (Supplementary Fig. 10) showed the presence of an oxidized statin residue (PreSta), with the hydroxy group converted into ketone group (δC-3 204.9). In addition, a decarboxylated and oxidized statin residue (DecPreSta) was identified. Finally, two valine, one alanine, and one acetyl group were identified. HMBC correlations together with MS/MS analysis determined the amino acid sequence, hence the planar structure of 9 was characterized.
Similarly, careful analysis of the NMR spectra (Supplementary Figs. 48−62, Supplementary Table 9) and MS/MS data (Supplementary Fig. 10) of compounds 10-12 showed they are the decarboxylated and oxidized intermedium of 2-3, respectively. Hence, the structures of compounds 10-12 were determined.
The molecular formula of 13 was determined to be C_30_H_55_N_5_O_7_ by High-resolution ESI-MS, m/z 598.4179 [M + H]^+^ (calcd. for C_30_H_56_N_5_O_7_, 598.4174). The NMR data (Supplementary Figs. 63−67, Supplementary Table 10) and MS/MS fragmentation data (Supplementary Fig. 16) indicated that the structure of 13 was similar to that of 9. The only difference is the PreSta residue in 9 was replaced by Sta residue in 13, indicated by the disappearance of one ketone signal (δC-3 204.9) and the appearance of one methine group (δH-3 3.84, δC-3 68.7).
Compound 17 had the molecular formula C_30_H_57_N_5_O_7_, m/z 600.4332 [M + H]^+^ (calcd. for C_30_H_58_N_5_O_7_, 600.4331). Compare the 1D and 2D NMR spectra (Supplementary Figs. 68−72, Supplementary Table 10) of 17 and 13 revealed that the ketone signal (δC-2 207.9) in 13 was replaced by the methine group (δH-2 3.56, δC-2 67.2) in 17. The structure of 17 was determined.
Crystallization and structure determination of kvPepI
Crystals of kvPepI, kvPepI – F_420,_ kvPepI^H62A^, kvPepI^H62A^ – F_420,_ and kvPepI^Y122A^ – F_420_ were obtained at 18 °C in 30% (w/v) PEG 4000, 0.2 M Sodium acetate and 0.1 M Tris-Cl pH 8.5. For complex crystallization, the protein was incubated with excess F_420_ (1.5 mM) on ice overnight. Crystals were cryoprotected in mother liquor supplemented with 30% glycerol. The diffraction data was collected from a single crystal at 100 K at Petra III (Beamline: P11, DESY)^63,64^, processed using Xia2^65^ or XDS^66^, and the structure was determined using PHASER molecular replacement^67^ using AlphaFold model generated using Colab notebook^68,69^. The structure was manually rebuilt in COOT^70^, refined using PHENIX Refine^67^, and validated using MolProbity^71^. The images presented were created using PyMOL (Schrödinger) and LigPlot^+^^72^.
Modeling of PepI: compound 9 complex
A model of the complex between the biosynthetic precursor of pepstatin and substrate of PepI (compound 9) and the kvPepI protein was generated based on the solved crystal structure (vide supra, PDB ID 9GM0) after the unresolved flexible loop Gly191-Thr194 was modeled by AlphaFold^68,69^ using the molecular operating environment (MOE, chemical computing group)^73^ in a stepwise manner:
- The PDB file was loaded in MOE and the QuickPrep protein preparation procedure was applied with the following parameters: Tether strength for receptor = 30; Tether strength for ligand = 10; co-factor (F_420_) atoms were fixed; all other parameters were default.
- The structure of compound 9 was inserted into the active site by first building the β-keto amide motif (precursor of the statine motif, “PreSta3”) in the orientation where the carbonyl oxygen is occupying the position of His62-coordinated water (H_2_O570; ordered water molecule from the main text) and the α-carbon, which is attacked by the hydride (or deuteride) in close proximity to the reactive center of co-factor F_420_ in the only possible orientation, which would lead to generation of the observed enantiomer (S-product; see Supplementary Fig. 25).
- Growing of the peptidic structure of compound 9 into the pocket and orienting the hydrophobic side chains into hydrophobic pockets. The Steric constraints of the active site required to model a compound 9 in a loop/bent conformation with the loop occurring between Val1 and PreSta3 to remove clashes with the protein resulting in a U-shaped conformation.
- Removal of all clashing water or solvent molecules as well as further finetuning of the complex structure.
- A final QuickPrep step for localized energy minimization with the following parameters: Tether strength for receptor = 30; Tether strength for ligand = 10; co-factor (F_420_) atoms were fixed; all other parameters were default.
This yielded the proposed model for the interaction between PepI and the pepstatin precursor 9. Note that this model is an information-driven hypothesis, which shows a plausible orientation for enabling the generation of the S-product at residue 4 observed in the experimental studies highlighting that this enzyme-substrate complex is in principle possible and that the active site can accommodate compound 9 in this orientation. In general, coordinates for substrate atoms more distant to the β-keto statine precursor motif are characterized by ambiguities inherent to modeling efforts on highly flexible peptidic substrates.
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Source Data
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