Next Article in Journal
Heterologous Machine Learning for the Identification of Antimicrobial Activity in Human-Targeted Drugs
Previous Article in Journal
Antiproliferative Aspidosperma-Type Monoterpenoid Indole Alkaloids from Bousigonia mekongensis Inhibit Tubulin Polymerization
 
 
Search for Articles:
Title / Keyword
Author / Affiliation / Email
Journal
Article Type
 
 
Advanced Search
 
Section
Special Issue
Volume
Issue
Number
Page
 
Journals
Molecules
Volume 24
Issue 7
10.3390/molecules24071257
molecules-logo
Submit to this Journal Review for this Journal Propose a Special Issue
► Article Menu

Article Menu

share Share announcement Help format_quote Cite question_answer Discuss in SciProfiles thumb_up
...
Endorse textsms
...
Comment
first_page
settings
Order Article Reprints
Font Type:
Arial Georgia Verdana
Font Size:
Aa Aa Aa
Line Spacing:
Column Width:
Background:
Article

Structural Comparison of Enterococcus faecalis and Human Thymidylate Synthase Complexes with the Substrate dUMP and Its Analogue FdUMP Provides Hints about Enzyme Conformational Variabilities

by
Cecilia Pozzi
1,
Stefania Ferrari
2,
Rosaria Luciani
2,
Giusy Tassone
1,
Maria Paola Costi
2 and
Stefano Mangani
1,*
1
Department of Biotechnology, Chemistry and Pharmacy—Department of Excellence 2018-2020, University of Siena, via Aldo Moro 2, 53100 Siena, Italy
2
Department of Life Sciences, University of Modena and Reggio Emilia, Via Campi 103, 41125 Modena, Italy
*
Author to whom correspondence should be addressed.
Molecules 2019, 24(7), 1257; https://doi.org/10.3390/molecules24071257
Submission received: 11 March 2019 / Revised: 22 March 2019 / Accepted: 28 March 2019 / Published: 31 March 2019
(This article belongs to the Section Chemical Biology)
Browse Figures
Versions Notes

Abstract

:
Thymidylate synthase (TS) is an enzyme of paramount importance as it provides the only de novo source of deoxy-thymidine monophosphate (dTMP). dTMP, essential for DNA synthesis, is produced by the TS-catalyzed reductive methylation of 2′-deoxyuridine-5′-monophosphate (dUMP) using N5,N10-methylenetetrahydrofolate (mTHF) as a cofactor. TS is ubiquitous and a validated drug target. TS enzymes from different organisms differ in sequence and structure, but are all obligate homodimers. The structural and mechanistic differences between the human and bacterial enzymes are exploitable to obtain selective inhibitors of bacterial TSs that can enrich the currently available therapeutic tools against bacterial infections. Enterococcus faecalis is a pathogen fully dependent on TS for dTMP synthesis. In this study, we present four new crystal structures of Enterococcus faecalis and human TSs in complex with either the substrate dUMP or the inhibitor FdUMP. The results provide new clues about the half-site reactivity of Enterococcus faecalis TS and the mechanisms underlying the conformational changes occurring in the two enzymes. We also identify relevant differences in cofactor and inhibitor binding between Enterococcus faecalis and human TS that can guide the design of selective inhibitors against bacterial TSs.

1. Introduction

Thymidylate synthase (TS, EC 2.1.1.45) is a ubiquitous enzyme that catalyzes the reductive methylation of 2′-deoxyuridine-5′-monophosphate (dUMP) to 2′-deoxythymidyne-5′-monophosphate (dTMP) using N5,N10-methylenetetrahydrofolate (mTHF) as a cofactor. In cells, TS provides the only synthetic source of dTMP necessary for DNA biosynthesis. Indeed, TS inhibition halts the replication processes and induces apoptosis in rapidly dividing cells, which is an effect known as “thymineless death” [1]. Given its pivotal role in cell survival and proliferation, TS represents a validated target in anticancer and antibacterial chemotherapy; even though some bacteria express a further enzyme, the flavin dependent TS (FDTS), that is able to catalyze the same reaction. FDTS requires flavin adenine dinucleotide (FAD) and nicotinamide adenine dinucleotide phosphate (NADPH) to perform its action [2]. Important human pathogens, including Bacillus anthracis, Clostridium botulinum, and Mycobacterium species, encode for both TS and FDTS [2]. In other pathogenic strains, such as Enterococcus faecalis, only TS has been identified [2]. The development of TS inhibitors that can be used alone or in combination with FDTS targeting molecules is a promising strategy to generate new effective antibacterial drugs.
TS works as an obligate homodimer, having residues from both enzyme subunits that contribute to substrate binding in each catalytic site. TS subunits are characterized by two domains, known as large and small domains (LD and SD, respectively). The LD, showing a mixed α/β structure, represents the conserved core of the enzyme, whereas the SD is highly variable (in extension and structure) among the different organisms. The structures of TSs from various sources have been elucidated. Among them, only those from Enterococcus faecalis (EfTS) and humans (hTS) have shown relevant domain changes that have been connected with different functional states of the enzymes (Figure 1) [3,4,5]. hTS switches between the active and inactive conformation through extended structural rearrangements that involve the catalytic loop (residues 181–197) [3,6]. In the active conformation, the catalytic Cys195 participates in the enzyme active site, whereas in the inactive conformation, it is exposed on the dimer interface (Figure 1a). On the other hand, EfTS is characterized by the transition between the closed and open states (Figure 1b) [5]. In the former, the SD (residues 69–138) is fully ordered and contributes to create the cofactor binding site, whereas, in the latter, it is highly flexible and allows opening of the catalytic cavity (Figure 1b). Differently from the human enzyme, the open and closed states were identified within the same EfTS homodimer, leading to asymmetry between the two enzyme subunits [5]. This phenomenon is related to the so-called “half-site reactivity”, whose presence in all forms of TS is still matter of debate [7,8]. The transitions to the closed state in EfTS, and to the active conformation in hTS, are fundamental to create functional active sites in which dUMP can bind, followed by the cofactor [3,5]. According to the reaction mechanism, the thiol of the conserved catalytic cysteine (Cys197 and Cys195, in EfTS and hTS, respectively) attacks the carbon atom in position 6 (C6) on the nucleotide pyrimidine base. This leads to the formation of a covalent adduct (Scheme 1) [9,10]. The dUMP uracil carbon in position 5 (C5) is then activated to accept the methyl moiety (C11) and the hydride donated by mTHF.
In the present work, we report the structural characterization of EfTS in complex with the substrate dUMP and its analogue 5-fluoro-2′-deoxyuridine-5′-monophosphate (FdUMP). FdUMP is a known potent TS inhibitor [11], for which we measured a Ki towards EfTS in the nM range. In both structures, dUMP and FdUMP populate only one catalytic cavity of the enzyme dimer, providing new evidence to support the half-site reactivity model proposed for this TS enzyme [5]. Furthermore, the comparison with the structure of native EfTS shows that substantial changes are induced by substrate binding. The structural analysis was also extended to the human enzyme (48 % sequence identity), reporting its characterization in complex with the same molecules. Even though former studies described the interactions of FdUMP within the hTS active site [12,13], we observe significant differences in the inhibitor binding mode. The structural information achieved provides new clues to explain the mechanisms guiding the conformational switches in these enzymes, highlighting a prominent role of the dimer interface in inter-subunit communication. Furthermore, the structural comparison of human and EfTS shows the presence of non-conserved residues in their catalytic cavities, mainly involved in cofactor binding. This information is of key importance for the rational development of inhibitors able to selectively target EfTS without altering the activity of the counterpart enzyme in the human host.

2. Results and Discussion

2.1. EfTS in Complex with the Substrate dUMP and Its Analogue FdUMP

2.1.1. EfTS Overall Fold

EfTS has the constitutive dimeric quaternary structure typical of all TS enzymes [14]. The two independent EfTS dimers (A-B and C-D), present in the cell asymmetric unit (ASU), have essentially identical structures and show structural heterogeneity between subunits due to asymmetric ligand binding within the enzyme active sites (Figure 2). The structure of the “as prepared” EfTS (PDB id 3UWL), formerly characterized by us, revealed the presence of a folate derivative, constitutively populating one active site within each EfTS homodimer [5]. This cofactor analogue, interpreted as 5-formyl-6-tetrahydrofolate (5-FTHF), copurifies with the enzyme and generates asymmetry between the two enzyme protomers (vide infra, Figure 2). 5-FTHF is a metabolite of the folate cycle that naturally occurs in the cell [15]. In the homodimer, Arg177 and Arg178 from one EfTS subunit participate in the assembly of the active site of the partner subunit. In both complexes, subunits B and D are in the closed state, displaying the SD (residues 69–138) fully structured in five α-helices connected by short loops, with the active site hosting the 5-FTHF molecule (Figure 2). On the other hand, the partner subunits (A and C) adopt the open conformation, showing the SD partially ordered in only three α-helices. Due to disorder, residues 92–124 and 98–118, in the dUMP and FdUMP complexes, respectively, have been excluded from our models.

2.1.2. EfTS–dUMP Complex

The structure of EfTS in complex with the substrate dUMP was determined to be 1.75 Å resolution (Figure 2, Table S1). The cofactor-analogue (6S)-5-formyl-6-tetrahydrofolate (5-FTHF) is entrapped in the active sites of subunits B and D by the same tight network of interactions already observed in the substrate-free form of the enzyme (Figure S1) [5]. Moreover, in these subunits, the catalytic Cys197 is modified as S,S-(2-hydroxylethyl)thiocysteine (CME197, Figure 2a and Figure S1) by the reaction with β-mercaptoethanol (added to the protein buffer during the purification process [5]). In the partner subunits (A and C), the electron density of the catalytic Cys197 suggests that it had been oxidized to sulfenic acid (S-oxycysteine, CSX197 in Figure 3). Despite the oxidation of Cys197, the substrate dUMP populates the active site, showing its uracil moiety positioned just above the cysteine sulphur (C6–Sγ distance of ~3.7 Å) (Figure 3). In both chains, the substrate shows the same network of interactions (Figure 3). The dUMP phosphate is salt-bridged to Arg22, Arg217, Arg177’, and Arg178’ (the last two from the partner subunit) and it is further H-bonded to the hydroxyl of Ser218. The dUMP ribose hydroxyl is H-bonded to His258 and Tyr260. The uracil ketone oxygen in position 2 receives H-bonds from the backbone nitrogen of Asn220 and the amide nitrogen of Gln216. Furthermore, the amide moiety of Asn228 donates an H-bond to the uracil ketone in position 4 and receives an H-bond from the uracil nitrogen in position 3.
While subunits A and C where dUMP is bound display the open conformation, subunits B and D where 5-FTHF is bound are in the closed conformation. The structural comparison with the substrate-free subunits of the enzyme (PDB id 3UWL [5]) shows that meaningful changes occur upon dUMP binding (Figure 4). The most evident rearrangement concerns the flexible loop 18–26, which moves towards the catalytic cavity in the dUMP-bound subunits, exposing Arg22 inside the phosphate recognition pocket (Figure 4). The movement of Arg22, whose Cα shifts by ~5.8 Å, is fundamental to create the four-arginine cluster that anchors the dUMP phosphate in the substrate site. However, this conformation of the 18–26 loop resembles that observed in the closed state of the substrate-free enzyme (PDB id 3UWL), where 5-FTHF is bound and in which the four-arginine cluster is fully formed and binds a sulfate/phosphate anion [5] (Figure 4). On the contrary, in the subunits of the substrate-free enzyme in the open conformation (subunits A and C of 3UWL), the loop is turned away from the active site and Arg22 points to the solvent-exposed surface of EfTS (Figure 4).
Remarkably, despite the full occupancy of the substrate site by dUMP and the movement of the 18–26 loop towards dUMP, the SD retains the open conformation, in which it is widely unstructured. This observation strongly suggests that in EfTS, the open/closed transition occurs as a biphasic process in which the dUMP accommodation triggers the closure of the loop 18–26, whereas the binding of the cofactor (or analogue) induces the movement and the organization of the whole SD.

2.1.3. EfTS–FdUMP Complex

Inhibition assays of EfTS activity performed on FdUMP resulted in a Ki of 74 nM. The structure of EfTS in complex with the substrate analogue FdUMP was determined at 2.88 Å resolution (Table S1), consistently showing subunit asymmetry within each enzyme dimer (Figure 2b). FdUMP populates the active sites of subunits B and D (Figure 5a) turned to a closed state, whereas chains A and C remain in the open conformation typical of ligand-free subunits (Figure 2b) [5]. In subunits B and D, FdUMP binding is accompanied by the accommodation of 5-FTHF in the cofactor site (the same cofactor analogue also entrapped in the active site of the native enzyme [5]; Figure 5a). FdUMP occupies the substrate pocket, where it mimics the dUMP binding mode, forming similar interactions within the cavity (Figure 3 and Figure 5a). Nonetheless, the 5-fluoro-uracil moiety of FdUMP is positioned closer to the catalytic Cys197 (distance of ~2.7 Å between the inhibitor C6 and the cysteine thiol) (Figure 5b). The shortening of this distance is possibly related to the different oxidation states of the catalytic cysteine, observed in the two complexes. Notably, in the dUMP-complex, the Cys197 side chain is modified to sulfenic acid, thus blocking the nucleophilic attack of the thiol to the substrate C6. On the contrary, in the complex with FdUMP, the thiol of Cys197 is reactive and can form a covalent adduct with the inhibitor that, indeed, is positioned closer to the catalytic residue. In this arrangement, the 5-fluorine on the FdUMP uracil moiety is proximal (~2.7 Å) to the Tyr145 hydroxyl, suggesting the formation of a halogen bond with it [16] (Figure 5a). Moreover, the same moiety of Tyr145 donates an H-bond to the FdUMP ketone oxygen in position 4, contributing to stabilize the inhibitor within the catalytic cavity.
At variance with the dUMP-complex, FdUMP binding is further stabilized by 5-FTHF (Figure 5a). Indeed, the pteridin moiety of 5-FTHF is accommodated just above the 5-fluoro-uracil of the substrate analogue, placing its 5-formyl substituent proximal to the FdUMP C5 (distance of ~3.2 Å). This configuration of the active site mimics the stage of the catalytic reaction in which the methyl moiety on the cofactor N5 (resulting from the aperture of the mTHF five-membered ring) is ready to be transferred to the substrate [9]. The structural comparison of the present ternary complex with the “as prepared” EfTS, where 5-FTHF alone populates the active site of one dimer subunit [5], shows that the binding mode of 5-FTHF is altered by bound FdUMP (Figure 5c). Notably, in the former EfTS structure, the catalytic Cys197 is modified to S,S-(2-hydroxylethyl)thiocysteine by the reaction with β-mercaptoethanol, allowing the 5-FTHF formyl moiety to protrude in the uracil pocket (Figure 5c). In contrast, the binding of FdUMP to the substrate site induces a rearrangement of 5-FTHF, whose 5-formyl group shifts by ~1.5 Å away from the inhibitor FdUMP (Figure 5c).

2.2. hTS in Complex with the Substrate dUMP and Its Analogue FdUMP

2.2.1. hTS Overall Fold

hTS was crystallized in the low-salt conditions (see Materials & Methods section; [4]), in the presence of either dUMP or FdUMP. In both complexes, the two subunits of the hTS homodimer adopt the active conformation, showing that Cys195 is exposed to the catalytic cavity, as occurs in previously reported structures [3,17]. The one and half homodimers found in the ASU were fully traced, apart for the first twenty-five N-terminal residues (and the twelve residues belonging to the non-removable His6-tag).

2.2.2. hTS–dUMP Complex

The structure of hTS in complex with dUMP was determined to 1.95 Å resolution (Table S1), providing a clear picture of substrate binding within the catalytic cavity (Figure 6a). The dUMP phosphate is salt bridged to the four arginines, Arg50, Arg215, Arg175’, and Arg176’ (the last two from the partner subunit), and it further receives an H-bond from Ser216 (Figure 6a). The dUMP ribose hydroxyl is H-bonded to His256 to Tyr258. The uracil ketone oxygen in position 2 receives two H-bonds from the backbone nitrogen of Asn218 and the amide nitrogen of Gln216. Nearby, the amide of Asn226 receives an H-bond from the dUMP uracil N3 and donates one to the ketone O4. The thiol of the catalytic Cys195 is located in an optimal position to attack the uracil C6 of the substrate (interatomic distances ranging from 3.14 Å to 3.27 Å in the three enzyme subunits). The dUMP binding mode and its interactions within the catalytic cavity are conserved with respect to those formerly described in binary and ternary complexes of hTS [17].

2.2.3. hTS–FdUMP Complex

The structure of hTS in complex with the substrate analogue FdUMP (Ki of 1.1 nM [18]) was determined to 2.08 Å resolution (Table S1). FdUMP fully occupies the hTS active site, perfectly mimicking the interactions entailed by dUMP in the substrate pocket (Figure 6). The 5-fluorine of FdUMP forms an additional water-mediated interaction with the Tyr135 hydroxyl (Figure 6b). FdUMP C6 is positioned 3.09–3.29 Å away from the Cys195 thiol, which is the same distance observed in the dUMP complex. Former structural analysis of the hTS variant R163K, showed that FdUMP adopts a slightly different orientation inside the substrate pocket (PDB id 3H9K [13]) (Figure 6c). Both the ribose and the 5-fluoro-uracil moieties of FdUMP are rotated by ~40° with respect to the orientations observed by us in the complex with the wt-enzyme, resulting in a remarkable loss of interactions with the surrounding residues inside the cavity (Figure 6c). Due to this rotation, the FdUMP C6 moves away from the Cys195 thiol in the R163K variant (distance of ~4.7 Å), far from the productive position, leading to the formation of the covalent adduct. Reasonably, the mutation of residue 163, located ~16 Å away from the catalytic cavity, is not responsible for these changes. Additionally, the hTS V3F variant-FdUMP complex has been reported (PDB id 3EJL [12]), showing that the substrate analogue is rotated outside the catalytic cavity (Figure 6c). In this configuration, FdUMP is directed towards the solvent-exposed surface of the enzyme with C6 placed ~12.0 Å away from the catalytic cysteine. The FdUMP binding modes observed in the complexes of the above hTS variants are not fully consistent with the mechanism of action of the inhibitor, relying on the formation of a covalent adduct with the TS catalytic cysteine [19]. On the other hand, in our complex, FdUMP mimics the substrate, placing its 5-fluoro-uracil C6 in an optimal position to form the covalent adduct with the reactive thiol of Cys195.

2.3. Structural Comparison between Bacterial and the Human TSs in Complex with dUMP and FdUMP

The structures of several bacterial TS–substrate complexes have been reported in the PDB (Escherichia coli TS, EcTS, PDB id 1BID [20]; Lactobacillus casei, LcTS, PDB id 2TDM [21]; Staphylococcus aureus TS, SaTS, PDB id 4DQ1 (unpublished results); Mycobacterium tuberculosis TS, MtbTS, PDB id 3QJ7 (unpublished results); Corynebacterium glutamicum TS, CgTS, 4H0U (unpublished results). The sequence alignment is displayed in Figure S2) and shows a remarkable conservation of the residues involved in dUMP binding. Figure 7a shows the superimposition of dUMP in EfTS, LcTS, and hTS, highlighting the same pose of the substrate in all enzymes. At variance with the other complexes, in EfTS, the catalytic Cys197 is oxidized in those subunits where dUMP is bound, evidencing that the residue modification does not alter the ability of the enzyme to accommodate the substrate. However, this explains the tiny gain in the distance between the uracil C6 and the cysteine thiol, resulting in ~3.7 Å in EfTS, whereas distances of 3.2–3.4 Å characterize other bacterial TS–dUMP complexes [20,21]. In all complexes, the four-arginine cluster, anchoring the dUMP phosphate, is highly conserved. This evidence strongly suggests that the closure of the loop 18–26, observed in EfTS upon dUMP binding, is important to stabilize the substrate inside the active site.
On the other hand, a slightly different configuration is observed in the complex with the substrate analogue FdUMP, which populates the catalytic cavity of EfTS together with the cofactor derivative 5-FHTF (Figure 7b). The ternary complex observed in EfTS is remarkably similar to the structure of MtbTS in complex with FdUMP and the cofactor 5-methyl-THF (deriving from aperture of the mTHF 5-membered ring; PDB id 4FOG, unpublished results) (Figure 7b). FdUMP adopts the same binding mode in both complexes, showing its uracil C6 positioned ~2.7 Å away from the thiol of the catalytic cysteine (Cys197 in EfTS, Cys146 in MtbTS). However, the 5-fluorine of the inhibitor is observed in two different orientations, being directed towards the cofactor in MtbTS, whereas in EfTS, it points towards the hydroxyl of Tyr145, allowing the formation of a halogen bond with it. Conserved binding modes also characterize the cofactor 5-methyl-THF and its analogue 5-FTHF, bound to MtbTS and EfTS. In each instance, the pterin N5 is positioned on top of FdUMP uracil C5. On the other hand, a slightly different configuration inside the catalytic cavity is displayed by the analogous complexes (FdUMP and 5-methyl-THF) obtained with Bacillus subtilis TS (BsTS; PDB id 1B02 [22]) and E. coli TS (PDB id 1TLS [23]). The structure of BsTS is reported in Figure 7b. In both structures, the formation of the ternary covalent adduct is observed, resulting from the covalent anchoring of the FdUMP C6 to the cysteine thiol and of the FdUMP C5 to the cofactor 5-methyl moiety. In the ternary covalent adducts, both ligands are slightly distorted. In EfTS, 5-FTHF, having a 5-formyl group that replaces the methyl of the cofactor, acts as an inhibitor, preventing the formation of the ternary covalent adduct. Therefore, our EfTS-FdUMP-5-FTHF ternary complex mimics the pre-reactive step of catalysis in which both substrate and cofactor are aligned in the cavity to allow the transfer of the pterin N-5 substituent.
The structure of the EfTS–FdUMP complex was also compared to that of the human enzyme, evidencing the occurrence of tiny changes in the inhibitor binding mode (Figure 7c). In EfTS, the FdUMP 5-fluorine is close to the Tyr145 hydroxyl, forming a halogen bond with it (Figure 5a and Figure 7c). In contrast, in the hTS complex, the FdUMP uracil is shifted far from the isostructural Tyr135, and a water molecule mediates its interaction with the fluorine of the inhibitor (Figure 6b and Figure 7c). A comparison of EfTS and hTS complexes shows that, in hTS, the orientation of His196 prevents the inhibitor from lying closer to Tyr135, whereas in EfTS, the sidechain of His198 (corresponding to hTS His196) is rotated by ~70°, allowing the direct interaction between the fluorine and Tyr145 (Figure 7c). The superimposition further evidences that FdUMP in hTS partially overlaps the cofactor site of EfTS. In addition, hTS Cys195 is slightly moved with respect to the position of the corresponding residue observed in EfTS. To explain these differences, the structure of EfTS was compared to the that of hTS in complex with dUMP and the cofactor analogue raltitrexed (PDB id 1HVY [3]), evidencing that even the cofactor site is somewhat shifted in the human enzyme (Figure 7d). Notably, in EfTS, the indole system of Trp84, belonging to the SD, protrudes inside the catalytic cavity and establishes van der Waals interactions with the cofactor analogue, generating a hindrance that induces a more compact assembly of FdUMP and 5-FTHF within the active site (Figure 7d). In hTS, Asn112 matches the position EfTS Trp84, allowing a less tight configuration inside the catalytic cavity (Figure 7d). This tryptophan residue of EfTS is conserved among bacterial TSs of other human pathogens, including S. aureus, B. melitensis, and Mycobacterium tuberculosis (Figure S2). The presence of Trp in bacterial TS versus Asn in the active site of hTS can be of key importance for the design of selective bacterial TS inhibitors.

2.4. Conformational Transitions in EfTS and hTS Enzymes

The structural studies performed on both E. faecalis and human TS highlighted the existence of different stable conformations that were connected to distinct functional states of the enzymes. Even though various hypotheses have been formulated, the mechanisms behind these conformational transitions have not been fully elucidated. In EfTS, the open and closed states characterize the two subunits of a single protein dimer (asymmetric homodimers), suggesting that this enzyme works through half-site reaction mechanisms [5]. Half-site reactivity, although with much less evident conformational changes, has also been reported for other bacterial TSs that differ in structure from EfTS [7,8]. On the other hand, conformational transitions are also characteristic of the human enzyme in which the active and inactive conformations are instead concomitantly adopted by both enzyme subunits, resulting in a symmetric homodimer.
The characterization of EfTS in complex with dUMP provides evidence that the transition between the open and the closed state occurs in this enzyme as a bi-phasic process. dUMP binding inside the catalytic cavity triggers the closure of the loop 18–26, exposing Arg22 inside the catalytic site, in which it participates in the four-arginines cluster that anchors the dUMP phosphate group. Remarkably, the binding of the substrate does not influence the whole SD that keeps the open conformation. Moreover, the movement of the 18–26 loop does not affect the partner subunit, where 5-FTHF is bound, which adopts the closed conformation. The flexibility of the 18–26 loop is a peculiar feature of EfTS; indeed, there is no evidence of analogous rearrangements in other TS enzymes.
On the other hand, the conformational transitions that characterize hTS do not involve loop 26–54, corresponding to the EfTS loop 18–26, which is oriented towards the catalytic cavity in both hTS active and inactive conformations. hTS is characterized by the high flexibility of the catalytic loop (residues 181–197) that shifts between the active and the inactive conformations. In the inactive conformation, the catalytic Cys195 moves out from the catalytic cavity into the enzyme dimer interface. The active conformation of the hTS catalytic loop closely resembles the orientation of the corresponding residues 183–199 in EfTS. It is worth noting that conformational transitions in both enzymes involve the SD, which shifts from a flexible to ordered structure. Both the open state of EfTS and the inactive conformation of hTS are characterized by widely unstructured SDs, which become fully orderered after the transition to the closed state and active conformation, respectively.
The structural comparison of these enzymes further evidences a common orientation for Gln148 in the EfTS closed state and for the corresponding Gln138 in the hTS active conformation (Figure 8). Notably, the side chains of both residues flip by ~180° following the transition to the open state and inactive configurations (Figure 8). In the EfTS closed state, the amide moiety of Gln148 is H-bonded to Asn143, Asn185, and Asp188 (Figure 8a). All these interactions are lost in the open state, in which the side chain of Gln148 is rotated away from these residues (Figure 8a). In EfTS, Asn185 and Asp188 belong to a loop located at the dimer interface, whose placement is also affected by the enzyme conformational transitions. Indeed, in the open state, Gln148 rotation releases the loop 183–199, which shifts towards the partner subunit by ~2.7 Å, whereas it is tied to Gln148 in the closed state. Furthermore, the EfTS residues 183–199 directly participate in the interface interaction with the partner subunit, suggesting that they can be involved in the inter-subunit communication, regulating the half-site reactivity that characterize this enzyme.
Analogously to the closed state of EfTS, in the active conformation of hTS, Gln138 forms conserved interactions with Pro133, Asn183, and Asp186 (Figure 8b). In contrast, the transition to the inactive conformation induces a flip of the Gln138 amide moiety, which loses its interactions with residues 183 and 186, but forms H-bonds with the backbone of Trp181 (Figure 8b). In hTS, residues 181–197 belong to the catalytic loop, highlighting the importance of the rearrangement of the Gln138 side chain to stabilize both conformations. It is worth noting that the portion 181–190 participates in the dimer interface, suggesting that the mobility of the catalytic loop also mediates the inter-subunit communication in hTS.

3. Materials and Methods

3.1. Macromolecule Production

EfTS was prepared according to an established procedure [5]. Human TS was expressed and purified as previously described, with minor modifications [24]. Briefly, hTS was expressed as the His6-tag protein (the not-cleavable N-terminal His6-tag was encoded by the pQE-80L expression plasmid) in E. coli strain BL21(DE3). Bacteria were cultured at 30 °C in the auto-induction medium ZYP-5052 [25] for 30 h. Cells, harvested by centrifugation (3000× g, 15 min, 8 °C), were suspended in buffer A (50 mM HEPES, pH 7.5, and 30 mM NaCl), with the addition of 20 mM imidazole, 0.2 mM phenylmethylsulfonyl fluoride (PMSF), and 0.5 mg mL−1 lysozyme, and then disrupted by sonication after 60 min incubation on ice. The cell-free extract, obtained by centrifugation (12,000× g, 60 min, 8 °C), was applied to a HisTrap HP 5 mL column (GE Healthcare, Chicago, IL, USA) and eluted using a 250–500 mM imidazole concentration in the same buffer. Fractions containing the target protein were pooled and dialyzed in buffer A. The high purity (>98%) of the resulting protein sample was confirmed by SDS-PAGE analysis and MALDI-TOF mass spectrometry.

3.2. Enzyme Activity and Inhbition Assayes

Enzyme activity assays were performed spectrophotometrically, according to a reported protocol [5,24]. Briefly, 1 mL reaction mixtures were prepared by adding aliquots of the enzyme (80–120 nM) to the assay buffer (50 mM TES, pH 7.4, 25 mM MgCl2, 6.5 mM HCHO, 1 mM EDTA, 75 mM β-mercaptoethanol), including variable concentrations of dUMP (50–200 μM) and mTHF (50–200 μM). Reactions, started by the addition of the substrate, were monitored by following the increase in absorbance at 340 nm during the oxidation reaction of mTHF to 7,8-dihydrofolate (DHF), for 3 min. Kinetic parameters characterized for both enzymes were in complete agreement with those formerly reported [5,24]. Inhibition assays for FdUMP were performed under the above condition using an enzyme concentration of 95 μM, and substrate and cofactor concentrations of 120 and 50 μM, respectively. The inhibition data versus hTS were already reported in the literature and were confirmed by our experiments [18]. The dose-response curve for EfTS inhibition by FdUMP was generated by adding compound concentrations ranging from 0.25 to 10 μM. The IC50 value, obtained by non-linear regression fitting of the initial rates (in terms of residual enzyme activity) versus the logarithm of the inhibitor concentrations, resulted in 0.815 ± 0.099 μM (as calculated using the software GraphPad Prism 8, San Diego, CA, USA). Measures were performed in triplicate. The Ki value of 74 nM for FdUMP versus EfTS was calculated using the equation IC50 = Ki (1 + S/KM) [26] (where S and KM are the substrate concentration and the Michaelis-Menten constant, respectively).

3.3. Protein Crystallization

3.3.1. EfTS

EfTS crystallization was performed using the hanging drop vapour-diffusion method [27] at room temperature. Crystals of the complex EfTS–dUMP were grown in drops prepared by mixing 4 μL of sample (EfTS 7 mg mL−1 in 25 mM phosphate buffer, pH 6.8, 100 mM dUMP, and 2 mM DTT) and 2 μL of precipitant (2.2–2.5 M ammonium sulfate and 0.1 M HEPES, pH 7.5) solutions and equilibrated over an 800 μL reservoir. Crystals of EfTS in complex with FdUMP were grown using the Nextal Crystallization Tool [28]. Drops were prepared by mixing equal volumes of sample (EfTS 7 mg mL−1 in 25 mM phosphate buffer, pH 6.8, 4 mM FdUMP, and 2 mM DTT) and the above precipitant solution and were equilibrated over a 1 mL reservoir. Before data collection, crystals (grown within two-three weeks) were transferred to the cryoprotectant solution (20 % vol/vol ethylene glycol, 2.5 M ammonium sulfate and 0.1 M HEPES, pH 7.5) and flash frozen in liquid nitrogen.

3.3.2. hTS

Crystals of hTS were grown at room temperature using the hanging-drop vapor-diffusion method [27]. Drops were prepared by mixing equal volumes of sample (hTS 20 mg mL−1 in 50 mM HEPES, pH 7.5, 30 mM NaCl, 20 mM β-mercaptoethanol, and either 40 mM dUMP or 2 mM FdUMP) and precipitant (27–30 % wt/vol PEG4000, 30 mM ammonium sulfate and 0.1 M TRIS, pH 9) solutions. Crystals appeared in one to three days in drops equilibrated over an 800 μL reservoir. Before data collection, crystals were washed in the cryoprotectant solution (20 % vol/vol PEG400, 30 % wt/vol PEG4000, 30 mM ammonium sulfate and 0.1 M TRIS, pH 9) and flash frozen in liquid nitrogen.

3.4. Data Collection and Processing, Structure Solution and Refinement

X-ray crystallographic data were collected using synchrotron radiation at the Diamond Light Source (DLS, Didcot, United Kingdom) beamlines I03, I04-1, and I24, equipped with either Dectris Pilatus 6M-F or Pilatus3 6M detectors, and at the PetraIII (DESY, Hamburg, Germany) beamline P14 on a Dectris Pilatus 6M-F detector. Reflections were indexed and integrated using the program Mosflm [29] and scaled with SCALA [30] from the CCP4 suite [31]. Data collection and reduction statistics are displayed in Table S1. EfTS crystals belonged to the primitive monoclinic space group P21, with two enzyme dimers in the cell asymmetric unit (ASU). hTS crystals are monoclinic, space groups C2 or I2, with three enzyme subunits in the ASU (one and half hTS dimer). In this case, one hTS dimer sits on a space group special position of multiplicity 2 (two-fold axis).
The structures of the complexes were solved by molecular replacement using the software Molrep [32] from the CCP4 suite. One monomer of hTS in the active conformation (PDB id 1HWY [3]) and a functional EfTS dimer (PDB id 3UWL [5]) were used as searching models, excluding water molecules and non-protein atoms. All structures were refined with Refmac5 [33] from the CCP4 suite using TLS parametrization [34] in the last cycles of the refinement protocol. The optimal partitioning of the polypeptide chains was calculated though the TLS Motion Determination web server [35], resulting in twenty continuous segments. The molecular graphic software Coot [36,37] was used for the manual rebuilding and modelling of missing atoms. Water molecules were added through the ARP/wARP suite [38] and checked with Coot. In all models, the occupancies of the exogenous ligands were adjusted to values resulting in atomic displacement parameters close to those of neighboring protein atoms in fully occupied sites. The stereochemical quality of the final models was checked using Coot and Procheck [39]. The overall quality of each structure has been validated though the Protein Data Bank submission procedure. Refinement statistics are reported in Table S2. Figures were generated using the molecular-graphic software CCP4mg [40].

3.5. PDB Deposition

Atomic coordinates and structure factors were deposited in the Protein Data Bank under the accession codes 6QYA (EfTS–dUMP), 6QXS (EfTS–FdUMP), 6QXH (hTS–dUMP), and 6QXG (hTS–FdUMP).

4. Conclusions

Enterococci are Gram-positive bacteria intrinsically resistant to various classes of antimicrobials [41,42]. In healthy people, E. faecalis, together with E. faecium, are only responsible for occasional urinary tract infections; however, they are deeply involved in healthcare-associated opportunistic infections. In recent years, vancomycin-resistant E. faecalis and E. faecium have become a serious health issue, highlighting the need to identify new antibiotics effective towards their infections. Bacterial TS enzymes represent a validated target for the development of antimicrobial drugs. In the past years, various classes of inhibitors have been explored for bacterial TSs, some of them specifically targeting Enterococcus faecalis TS, such as phtalimide-derivatives [43,44]. The most active phtalimide inhibitors of EfTS showed selectivity towards the human counterpart enzyme [44]. Nevertheless, much larger efforts are required to achieve effective treatments. EfTS is characterized by a quite peculiar behaviour, being the only bacterial TS known so far showing large asymmetry within each enzyme dimer. This has been associated with the alternate transitions between the open and closed states of its subunits. In this work, we provide new evidence to support the half-site reactivity model proposed for this enzyme. Indeed, asymmetrical ligand binding is observed in EfTS complexes with both the substrate dUMP and its analogue FdUMP. Furthermore, these complexes provide new important insight into the mechanism concerning the transition between the open and closed states, providing evidence that it occurs in EfTS as a bi-phasic process. The binding of the dUMP substrate triggers the closure of the loop 18–26, whereas the rearrangement of the SD, required to complete the transition to the closed state, needs the population of the cofactor site. This is particularly evident in the complex with FdUMP, in which the settlement of the substrate pocket is accompanied by the binding of 5-FTHF in the cofactor site. However, in EfTS-dUMP and EfTS-FdUMP complexes, the concomitant population of the substrate site in both dimer subunits was not observed. The reason behind this unique behaviour of EfTS remains an open question.
The comparison with the analogous complexes obtained for the human enzyme highlights meaningful differences in ligand binding. In EfTS, Trp84 displays a major contribution to cofactor binding, inducing a more compact assembly of the molecules in the catalytic cavity. On the other hand, hTS Asn112 matches the position of EfTS Trp84, generating a rearrangement of both the cofactor and the substrate sites inside the cavity.
The structure of EfTS in complex with a representative phtalimide inhibitor (PDB id 4O7U [44]) showed close van der Waals contact between the six-membered aromatic ring of phtalimide and Trp84, explaining the selectivity profile of these molecules. Trp84 of EfTS is also conserved in TSs of other human pathogens, such as M. tuberculosis and S. aureus, providing a clue for the design of new selective bacterial TSs inhibitors.

Supplementary Materials

Figure S1: structural comparison of the 5-FTHF binding mode; Figure S2: Sequence alignment among TSs from different sources; Table S1: Data collection and processing statisctics; Table S2. Structure solution and refinement statistics.

Author Contributions

Protein expression and purification, R.L. and C.P.; enzyme kinetics and inhibition assays, G.T.; protein crystallization, crystallographic data collection and crystal structure solution and refinement, C.P.; writing and original draft preparation, C.P. and S.M.; writing, review, and editing, S.F., M.P.C., C.P., and S.M.

Funding

To access the synchrotron facilities, we received financial support from the European Community’s Seventh Framework Programme (FP7/2007–2013) under BioStruct-X (grant agreement No. 283570).

Acknowledgments

We thank the synchrotron facilities Diamond Light Source and PetraIII for providing access to the beamlines I03, I04-1, and I24 (DLS proposal No. BIOSTRUCTX_1358), and P14 (PetraIII proposal No. BIOSTRUCTX_1358), respectively. Authors would also like to acknowledge the staff of the synchrotron sources for their assistance in using the beamlines.

Conflicts of Interest

The authors declare no conflict of interest. The funders had no role in the design of the study; in the collection, analyses, or interpretation of data; in the writing of the manuscript, or in the decision to publish the results.

References

  1. Houghton, J.A.; Houghton, P.J. Cellular responses to antimetabolite anticancer agents: Cytostasis versus cytotoxicity. In Progress in Cell Cycle Research; Springer: Boston, MA, USA, 1996; pp. 175–185. ISBN 978-1-4613-7693-4. [Google Scholar]
  2. Choi, M.; Karunaratne, K.; Kohen, A. Flavin-Dependent Thymidylate Synthase as a New Antibiotic Target. Molecules 2016, 21, 654. [Google Scholar] [CrossRef]
  3. Phan, J.; Koli, S.; Minor, W.; Dunlap, R.B.; Berger, S.H.; Lebioda, L. Human Thymidylate Synthase Is in the Closed Conformation When Complexed with dUMP and Raltitrexed, an Antifolate Drug. Biochemistry 2001, 40, 1897–1902. [Google Scholar] [CrossRef]
  4. Lovelace, L.L.; Minor, W.; Lebioda, L. Structure of human thymidylate synthase under low-salt conditions. Acta Crystallogr. D Biol. Crystallogr. 2005, 61, 622–627. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  5. Pozzi, C.; Ferrari, S.; Cortesi, D.; Luciani, R.; Stroud, R.M.; Catalano, A.; Costi, M.P.; Mangani, S. The structure of Enterococcus faecalis thymidylate synthase provides clues about folate bacterial metabolism. Acta Crystallogr. D Biol. Crystallogr. 2012, 68, 1232–1241. [Google Scholar] [CrossRef] [PubMed]
  6. Schiffer, C.A.; Clifton, I.J.; Davisson, V.J.; Santi, D.V.; Stroud, R.M. Crystal structure of human thymidylate synthase: A structural mechanism for guiding substrates into the active site. Biochemistry 1995, 34, 16279–16287. [Google Scholar] [CrossRef] [PubMed]
  7. Sapienza, P.J.; Falk, B.T.; Lee, A.L. Bacterial Thymidylate Synthase Binds Two Molecules of Substrate and Cofactor without Cooperativity. J. Am. Chem. Soc. 2015, 137, 14260–14263. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  8. Finer-Moore, J.S.; Lee, T.T.; Stroud, R.M. A Single Mutation Traps a Half-Sites Reactive Enzyme in Midstream, Explaining Asymmetry in Hydride Transfer. Biochemistry 2018, 57, 2786–2795. [Google Scholar] [CrossRef]
  9. Stroud, R.M.; Finer-Moore, J.S. Conformational dynamics along an enzymatic reaction pathway: Thymidylate synthase, “the movie”. Biochemistry 2003, 42, 239–247. [Google Scholar] [CrossRef]
  10. Kholodar, S.A.; Kohen, A. Noncovalent Intermediate of Thymidylate Synthase: Fact or Fiction? J. Am. Chem. Soc. 2016, 138, 8056–8059. [Google Scholar] [CrossRef] [Green Version]
  11. Costi, M.P.; Ferrari, S.; Venturelli, A.; Calò, S.; Tondi, D.; Barlocco, D. Thymidylate synthase structure, function and implication in drug discovery. Curr. Med. Chem. 2005, 12, 2241–2258. [Google Scholar] [CrossRef]
  12. Huang, X.; Gibson, L.M.; Bell, B.J.; Lovelace, L.L.; Peña, M.M.O.; Berger, F.G.; Berger, S.H.; Lebioda, L. Replacement of Val3 in human thymidylate synthase affects its kinetic properties and intracellular stability. Biochemistry 2010, 49, 2475–2482. [Google Scholar] [CrossRef] [PubMed]
  13. Gibson, L.M.; Celeste, L.R.; Lovelace, L.L.; Lebioda, L. Structures of human thymidylate synthase R163K with dUMP, FdUMP and glutathione show asymmetric ligand binding. Acta Crystallogr. D Biol. Crystallogr. 2011, 67, 60–66. [Google Scholar] [CrossRef] [PubMed]
  14. Carreras, C.W.; Santi, D.V. The Catalytic Mechanism and Structure of Thymidylate Synthase. Annu. Rev. Biochem. 1995, 64, 721–762. [Google Scholar] [CrossRef] [PubMed]
  15. Stover, P.; Schirch, V. The metabolic role of leucovorin. Trends Biochem. Sci. 1993, 18, 102–106. [Google Scholar] [CrossRef]
  16. Cavallo, G.; Metrangolo, P.; Milani, R.; Pilati, T.; Priimagi, A.; Resnati, G.; Terraneo, G. The Halogen Bond. Chem. Rev. 2016, 116, 2478–2601. [Google Scholar] [CrossRef] [Green Version]
  17. Chen, D.; Jansson, A.; Sim, D.; Larsson, A.; Nordlund, P. Structural analyses of human thymidylate synthase reveal a site that may control conformational switching between active and inactive states. J. Biol. Chem. 2017, 292, 13449–13458. [Google Scholar] [CrossRef]
  18. Cardinale, D.; Salo-Ahen, O.M.H.; Guaitoli, G.; Ferrari, S.; Venturelli, A.; Franchini, S.; Battini, R.; Ponterini, G.; Wade, R.C.; Costi, M.P. Design and characterization of a mutation outside the active site of human thymidylate synthase that affects ligand binding. Protein Eng. Des. Sel. 2010, 23, 81–89. [Google Scholar] [CrossRef]
  19. Longley, D.B.; Harkin, D.P.; Johnston, P.G. 5-Fluorouracil: Mechanisms of action and clinical strategies. Nat. Rev. Cancer 2003, 3, 330–338. [Google Scholar] [CrossRef]
  20. Stout, T.J.; Sage, C.R.; Stroud, R.M. The additivity of substrate fragments in enzyme–ligand binding. Structure 1998, 6, 839–848. [Google Scholar] [CrossRef] [Green Version]
  21. Finer-Moore, J.; Fauman, E.B.; Foster, P.G.; Perry, K.M.; Santi, D.V.; Stroud, R.M. Refined Structures of Substrate-bound and Phosphate-bound Thymidylate Synthase from Lactobacillus casei. J. Mol. Biol. 1993, 232, 1101–1116. [Google Scholar] [CrossRef]
  22. Fox, K.M.; Maley, F.; Garibian, A.; Changchien, L.-M.; Roey, P.V. Crystal structure of thymidylate synthase A from Bacillus subtilis. Protein Sci. 1999, 8, 538–544. [Google Scholar] [CrossRef]
  23. Hyatt, D.C.; Maley, F.; Montfort, W.R. Use of Strain in a Stereospecific Catalytic Mechanism:  Crystal Structures of Escherichia coli Thymidylate Synthase Bound to FdUMP and Methylenetetrahydrofolate. Biochemistry 1997, 36, 4585–4594. [Google Scholar] [CrossRef]
  24. Salo-Ahen, O.M.H.; Tochowicz, A.; Pozzi, C.; Cardinale, D.; Ferrari, S.; Boum, Y.; Mangani, S.; Stroud, R.M.; Saxena, P.; Myllykallio, H.; et al. Hotspots in an Obligate Homodimeric Anticancer Target. Structural and Functional Effects of Interfacial Mutations in Human Thymidylate Synthase. J. Med. Chem. 2015, 58, 3572–3581. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  25. Studier, F.W. Protein production by auto-induction in high density shaking cultures. Protein Expr. Purif. 2005, 41, 207–234. [Google Scholar] [CrossRef] [PubMed]
  26. Yung-Chi, C.; Prusoff, W.H. Relationship between the inhibition constant (KI) and the concentration of inhibitor which causes 50 per cent inhibition (I50) of an enzymatic reaction. Biochem. Pharmacol. 1973, 22, 3099–3108. [Google Scholar] [CrossRef]
  27. Benvenuti, M.; Mangani, S. Crystallization of soluble proteins in vapor diffusion for x-ray crystallography. Nat. Protoc. 2007, 2, 1633–1651. [Google Scholar] [CrossRef] [Green Version]
  28. Nneji, G.A.; Chayen, N.E. A crystallization plate for controlling evaporation in hanging drops. J. Appl. Crystallogr. 2004, 37, 502–503. [Google Scholar] [CrossRef] [Green Version]
  29. Powell, H.R.; Johnson, O.; Leslie, A.G.W. Autoindexing diffraction images with iMosflm. Acta Crystallogr. D Biol. Crystallogr. 2013, 69, 1195–1203. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  30. Evans, P. Scaling and assessment of data quality. Acta Crystallogr. D Biol. Crystallogr. 2006, 62, 72–82. [Google Scholar] [CrossRef] [PubMed]
  31. Winn, M.D.; Ballard, C.C.; Cowtan, K.D.; Dodson, E.J.; Emsley, P.; Evans, P.R.; Keegan, R.M.; Krissinel, E.B.; Leslie, A.G.W.; McCoy, A.; et al. Overview of the CCP4 suite and current developments. Acta Crystallogr. D Biol. Crystallogr. 2011, 67, 235–242. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  32. Vagin, A.; Teplyakov, A. Molecular replacement with MOLREP. Acta Crystallogr. D Biol. Crystallogr. 2010, 66, 22–25. [Google Scholar] [CrossRef]
  33. Murshudov, G.N.; Skubák, P.; Lebedev, A.A.; Pannu, N.S.; Steiner, R.A.; Nicholls, R.A.; Winn, M.D.; Long, F.; Vagin, A.A. REFMAC5 for the refinement of macromolecular crystal structures. Acta Crystallogr. D Biol. Crystallogr. 2011, 67, 355–367. [Google Scholar] [CrossRef] [Green Version]
  34. Winn, M.D.; Isupov, M.N.; Murshudov, G.N. Use of TLS parameters to model anisotropic displacements in macromolecular refinement. Acta Crystallogr. D Biol. Crystallogr. 2001, 57, 122–133. [Google Scholar] [CrossRef] [Green Version]
  35. Painter, J.; Merritt, E.A. TLSMD web server for the generation of multi-group TLS models. J. Appl. Crystallogr. 2006, 39, 109–111. [Google Scholar] [CrossRef]
  36. Emsley, P.; Cowtan, K. Coot: Model-building tools for molecular graphics. Acta Crystallogr. D Biol. Crystallogr. 2004, 60, 2126–2132. [Google Scholar] [CrossRef]
  37. Emsley, P.; Lohkamp, B.; Scott, W.G.; Cowtan, K. Features and development of Coot. Acta Crystallogr. D Biol. Crystallogr. 2010, 66, 486–501. [Google Scholar] [CrossRef] [PubMed]
  38. Langer, G.; Cohen, S.X.; Lamzin, V.S.; Perrakis, A. Automated macromolecular model building for X-ray crystallography using ARP/wARP version 7. Nat. Protoc. 2008, 3, 1171–1179. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  39. Laskowski, R.A.; MacArthur, M.W.; Thornton, J.M. Validation of protein models derived from experiment. Curr. Opin. Struct. Biol. 1998, 8, 631–639. [Google Scholar] [CrossRef]
  40. Potterton, L.; McNicholas, S.; Krissinel, E.; Gruber, J.; Cowtan, K.; Emsley, P.; Murshudov, G.N.; Cohen, S.; Perrakis, A.; Noble, M. Developments in the CCP4 molecular-graphics project. Acta Crystallogr. D Biol. Crystallogr. 2004, 60, 2288–2294. [Google Scholar] [CrossRef]
  41. Vu, J.; Carvalho, J. Enterococcus: Review of its physiology, pathogenesis, diseases and the challenges it poses for clinical microbiology. Front. Biol. 2011, 6, 357–366. [Google Scholar] [CrossRef]
  42. Sparo, M.; Delpech, G.; García Allende, N. Impact on Public Health of the Spread of High-Level Resistance to Gentamicin and Vancomycin in Enterococci. Front. Microbiol. 2018, 9, 3073. [Google Scholar] [CrossRef] [PubMed]
  43. Mangani, S.; Cancian, L.; Leone, R.; Pozzi, C.; Lazzari, S.; Luciani, R.; Ferrari, S.; Costi, M.P. Identification of the Binding Modes of N-Phenylphthalimides Inhibiting Bacterial Thymidylate Synthase through X-Ray Crystallography Screening. J. Med. Chem. 2011, 54, 5454–5467. [Google Scholar] [CrossRef] [PubMed]
  44. Catalano, A.; Luciani, R.; Carocci, A.; Cortesi, D.; Pozzi, C.; Borsari, C.; Ferrari, S.; Mangani, S. X-ray crystal structures of Enterococcus faecalis thymidylate synthase with folate binding site inhibitors. Eur. J. Med. Chem. 2016, 123, 649–664. [Google Scholar] [CrossRef] [PubMed]
Sample Availability: Samples of the compounds are not available from the authors.
Molecules 24 01257 g001 550
Figure 1. (a) Cartoon representation of the hTS homodimer in the active (PDB id 1HVY [3]) and inactive conformations (PDB id 1YPV [4]; for the inactive conformation, only the catalytic loop, including residues 181–197, is shown for clarity). In both subunits, the large and small domains are coloured light pink and dark pink, respectively. The two orientations of the catalytic loop (residues 181–197), defining the active (brown trace, PDB id 1HVY [3]) and inactive (green trace, PDB id 1YPV [4]) enzyme conformations, are displayed. The catalytic cysteine is shown in sticks (brown and green carbons in the active and inactive conformations, respectively). The position of the catalytic cavity is indicated by the presence of the substrate 2′-deoxyuridine 5′-monophosphate (dUMP, in sticks, black carbons). (b) Cartoon representation of the EfTS homodimer (PDB id 3UWL [5]). In both subunits, the large and small domains are coloured white and dark pink, respectively. The large domain (residues 1–68 and 139–315), representing the conserved core of the enzyme, shows an α/β structure generated by seven α-helices and eight β-strands. The small domain (residues 69–138) are only fully structured (five α-helices connected by short loops) in the enzyme subunit with the cofactor binding site populated by 5-formyl-6-tetrahydrofolate (5-FTHF, in sticks, purple carbons). In the partner subunit, the small domain is highly flexible and only partially visible in the structures. The position of the active site is indicated by the catalytic Cys197 (in sticks, white carbons; in subunit B, it is modified as S,S-(2-hydroxyethyl)thiocysteine, CME197). In all figures, nitrogen atoms are coloured blue, oxygen red, sulphur yellow, and phosphorous magenta.
Figure 1. (a) Cartoon representation of the hTS homodimer in the active (PDB id 1HVY [3]) and inactive conformations (PDB id 1YPV [4]; for the inactive conformation, only the catalytic loop, including residues 181–197, is shown for clarity). In both subunits, the large and small domains are coloured light pink and dark pink, respectively. The two orientations of the catalytic loop (residues 181–197), defining the active (brown trace, PDB id 1HVY [3]) and inactive (green trace, PDB id 1YPV [4]) enzyme conformations, are displayed. The catalytic cysteine is shown in sticks (brown and green carbons in the active and inactive conformations, respectively). The position of the catalytic cavity is indicated by the presence of the substrate 2′-deoxyuridine 5′-monophosphate (dUMP, in sticks, black carbons). (b) Cartoon representation of the EfTS homodimer (PDB id 3UWL [5]). In both subunits, the large and small domains are coloured white and dark pink, respectively. The large domain (residues 1–68 and 139–315), representing the conserved core of the enzyme, shows an α/β structure generated by seven α-helices and eight β-strands. The small domain (residues 69–138) are only fully structured (five α-helices connected by short loops) in the enzyme subunit with the cofactor binding site populated by 5-formyl-6-tetrahydrofolate (5-FTHF, in sticks, purple carbons). In the partner subunit, the small domain is highly flexible and only partially visible in the structures. The position of the active site is indicated by the catalytic Cys197 (in sticks, white carbons; in subunit B, it is modified as S,S-(2-hydroxyethyl)thiocysteine, CME197). In all figures, nitrogen atoms are coloured blue, oxygen red, sulphur yellow, and phosphorous magenta.
Molecules 24 01257 g001
Molecules 24 01257 sch001 550
Scheme 1. Proposed reaction scheme for the TS catalyzed reaction. Adapted from [9,10].
Scheme 1. Proposed reaction scheme for the TS catalyzed reaction. Adapted from [9,10].
Molecules 24 01257 sch001
Molecules 24 01257 g002 550
Figure 2. Dimer of EfTS (large and small domains are represented as grey and dark pink cartoon, respectively) in complex with (a) dUMP (in sticks, black carbons) and (b) FdUMP (in sticks, cyan carbons). Structural heterogeneity within the functional EfTS dimer is observed in both complexes. In the EfTS–dUMP complex, the nucleotide is bound to subunit A, whereas the cofactor-like molecule 5-formyl-6-tetrahydrofolate (5-FTHF, in sticks, purple carbons) occupies the active site of subunit B in which the catalytic cysteine is modified as S,S-(2-hydroxyethyl)thiocysteine (CME197, in sticks, grey carbons). On the other hand, in the EfTS–FdUMP complex, the substrate-like inhibitor (in sticks, cyan carbons) is bound to subunit B together with the cofactor-like molecule 5-FTHF (in sticks, purple carbons).
Figure 2. Dimer of EfTS (large and small domains are represented as grey and dark pink cartoon, respectively) in complex with (a) dUMP (in sticks, black carbons) and (b) FdUMP (in sticks, cyan carbons). Structural heterogeneity within the functional EfTS dimer is observed in both complexes. In the EfTS–dUMP complex, the nucleotide is bound to subunit A, whereas the cofactor-like molecule 5-formyl-6-tetrahydrofolate (5-FTHF, in sticks, purple carbons) occupies the active site of subunit B in which the catalytic cysteine is modified as S,S-(2-hydroxyethyl)thiocysteine (CME197, in sticks, grey carbons). On the other hand, in the EfTS–FdUMP complex, the substrate-like inhibitor (in sticks, cyan carbons) is bound to subunit B together with the cofactor-like molecule 5-FTHF (in sticks, purple carbons).
Molecules 24 01257 g002
Molecules 24 01257 g003 550
Figure 3. Active site view of EfTS (white cartoon and carbon atoms) in complex with dUMP (in sticks, black carbon atoms). In the panel, dUMP is surrounded by the omit map (green mesh) contoured at the 2.5 σ level. Key interactions (salt bridges, hydrogen and halogen bonds) are displayed as tan dashed lines. The catalytic cysteine is oxidized to sulfenic acid (S-oxycysteine, CSX197), surrounded by the 2Fo-Fc map (blue mesh, contoured at the 1.5 σ level).
Figure 3. Active site view of EfTS (white cartoon and carbon atoms) in complex with dUMP (in sticks, black carbon atoms). In the panel, dUMP is surrounded by the omit map (green mesh) contoured at the 2.5 σ level. Key interactions (salt bridges, hydrogen and halogen bonds) are displayed as tan dashed lines. The catalytic cysteine is oxidized to sulfenic acid (S-oxycysteine, CSX197), surrounded by the 2Fo-Fc map (blue mesh, contoured at the 1.5 σ level).
Molecules 24 01257 g003
Molecules 24 01257 g004 550
Figure 4. Structural comparison of the different states observed in the structure of substrate-free EfTS (PDB id 3UWL [5], open conformation in gold and closed conformation in light blue) and in its complex with dUMP (open conformation in white, only the dUMP-bound subunit is shown). The closed conformation of both SD (circled) and loop 18–26 is observed in subunits B and D of substrate-free EfTS (light blue cartoon and carbon atoms) where 5-FTHF is bound. The open conformation of SD and loop 18-26 is observed in chains A and C of the substrate-free enzyme (gold cartoon and carbons). In the EfTS–dUMP complex (in white), a closed conformation of loop 18–26 is visible in the dUMP-bound subunits. In EfTS, the open/closed transition occurs as a biphasic process in which the dUMP binding triggers the closure of loop 18–26 (pink dashed arrow), whereas the binding of the cofactor (or analogue) induces the movement and the organization of the whole SD (purple dashed arrow).
Figure 4. Structural comparison of the different states observed in the structure of substrate-free EfTS (PDB id 3UWL [5], open conformation in gold and closed conformation in light blue) and in its complex with dUMP (open conformation in white, only the dUMP-bound subunit is shown). The closed conformation of both SD (circled) and loop 18–26 is observed in subunits B and D of substrate-free EfTS (light blue cartoon and carbon atoms) where 5-FTHF is bound. The open conformation of SD and loop 18-26 is observed in chains A and C of the substrate-free enzyme (gold cartoon and carbons). In the EfTS–dUMP complex (in white), a closed conformation of loop 18–26 is visible in the dUMP-bound subunits. In EfTS, the open/closed transition occurs as a biphasic process in which the dUMP binding triggers the closure of loop 18–26 (pink dashed arrow), whereas the binding of the cofactor (or analogue) induces the movement and the organization of the whole SD (purple dashed arrow).
Molecules 24 01257 g004
Molecules 24 01257 g005 550
Figure 5. (a) Active site view of EfTS (white cartoon and carbon atoms) in complex with FdUMP (in sticks, cyan carbons) and 5-FTHF (in sticks, dark grey carbons). In the panel, FdUMP and 5-FTHF are surrounded by their omit map (green mesh) contoured at the 2.5 σ level. Key interactions (salt bridges, hydrogen and halogen bonds) are displayed as tan dashed lines. (b) View of the active site of EfTS in complex with dUMP (dUMP and CSX197 in sticks, black carbons) superimposed to the EfTS-FdUMP-5-FTHF complex (FdUMP, Cys197, and 5-FTHF in sticks, cyan carbons). (c) View of the active site of the EfTS–FdUMP-5-FTHF complex (FdUMP, Cys197, and 5-FTHF in sticks, cyan carbons) superimposed to the substrate-free EfTS (PDB id 3UWL, [5]; Cys197 modified as S,S-(2-hydroxyethyl)thiocysteine, CME-197 and 5-FTHF in sticks, purple carbons). Fluorine atoms are colored grey.
Figure 5. (a) Active site view of EfTS (white cartoon and carbon atoms) in complex with FdUMP (in sticks, cyan carbons) and 5-FTHF (in sticks, dark grey carbons). In the panel, FdUMP and 5-FTHF are surrounded by their omit map (green mesh) contoured at the 2.5 σ level. Key interactions (salt bridges, hydrogen and halogen bonds) are displayed as tan dashed lines. (b) View of the active site of EfTS in complex with dUMP (dUMP and CSX197 in sticks, black carbons) superimposed to the EfTS-FdUMP-5-FTHF complex (FdUMP, Cys197, and 5-FTHF in sticks, cyan carbons). (c) View of the active site of the EfTS–FdUMP-5-FTHF complex (FdUMP, Cys197, and 5-FTHF in sticks, cyan carbons) superimposed to the substrate-free EfTS (PDB id 3UWL, [5]; Cys197 modified as S,S-(2-hydroxyethyl)thiocysteine, CME-197 and 5-FTHF in sticks, purple carbons). Fluorine atoms are colored grey.
Molecules 24 01257 g005
Molecules 24 01257 g006 550
Figure 6. (a,b) Active site view of hTS (light pink cartoon and carbon atoms) in complex with (a) dUMP (in sticks, black carbon atoms) and (b) FdUMP (in sticks, cyan carbons). In both panels, the ligands are surrounded by the omit map (green mesh) contoured at the 2.5 σ level, and key interactions (salt bridges, hydrogen and halogen bonds) are displayed as tan dashed lines. (c) Different orientations of FdUMP in the complexes with the wild-type hTS (pink cartoon and carbon atoms, FdUMP in sticks, cyan carbons) and the variants R163K (FdUMP in sticks, dark green carbons; 3H9K [13]) and V3F (FdUMP in sticks, green carbons; PDB id 3EJL [12]).
Figure 6. (a,b) Active site view of hTS (light pink cartoon and carbon atoms) in complex with (a) dUMP (in sticks, black carbon atoms) and (b) FdUMP (in sticks, cyan carbons). In both panels, the ligands are surrounded by the omit map (green mesh) contoured at the 2.5 σ level, and key interactions (salt bridges, hydrogen and halogen bonds) are displayed as tan dashed lines. (c) Different orientations of FdUMP in the complexes with the wild-type hTS (pink cartoon and carbon atoms, FdUMP in sticks, cyan carbons) and the variants R163K (FdUMP in sticks, dark green carbons; 3H9K [13]) and V3F (FdUMP in sticks, green carbons; PDB id 3EJL [12]).
Molecules 24 01257 g006
Molecules 24 01257 g007 550
Figure 7. Active site view of the superimposition among the complexes: (a) EfTS–dUMP (CSX197 in sticks, white carbon atoms; dUMP in sticks, black carbons), LcTS–dUMP (in sticks, light green carbons; PDB id 2TDM [21]), and hTS–dUMP (in sticks, pink carbons). (b) EfTS–FdUMP–5-FTHF (Cys197 in sticks, white carbon atoms; ligands in sticks, cyan carbons), MtbTS–FdUMP–5-methyl-THF (in sticks, orange carbons; PDB id 4FOG, unpublished results), and BsTS–FdUMP–5-methyl-THF (in sticks, olive carbons; PDB id 1B02 [22]). (c) EfTS–FdUMP–5-FTHF (white cartoon, Cys197 in sticks, white carbon atoms; ligands in sticks, cyan carbons) and hTS–FdUMP (pink cartoon and carbon atoms). (d) EfTS–FdUMP–5-FTHF (white cartoons, Cys197 white carbon atoms; ligands in sticks, cyan carbons) and hTS–dUMP–raltitrexed (pink cartoon and carbon atoms). In the (a) and (b) panels, only the catalytic cysteine is shown in the structures of LcTS, hTS, MtbTS, and BsTS for clarity.
Figure 7. Active site view of the superimposition among the complexes: (a) EfTS–dUMP (CSX197 in sticks, white carbon atoms; dUMP in sticks, black carbons), LcTS–dUMP (in sticks, light green carbons; PDB id 2TDM [21]), and hTS–dUMP (in sticks, pink carbons). (b) EfTS–FdUMP–5-FTHF (Cys197 in sticks, white carbon atoms; ligands in sticks, cyan carbons), MtbTS–FdUMP–5-methyl-THF (in sticks, orange carbons; PDB id 4FOG, unpublished results), and BsTS–FdUMP–5-methyl-THF (in sticks, olive carbons; PDB id 1B02 [22]). (c) EfTS–FdUMP–5-FTHF (white cartoon, Cys197 in sticks, white carbon atoms; ligands in sticks, cyan carbons) and hTS–FdUMP (pink cartoon and carbon atoms). (d) EfTS–FdUMP–5-FTHF (white cartoons, Cys197 white carbon atoms; ligands in sticks, cyan carbons) and hTS–dUMP–raltitrexed (pink cartoon and carbon atoms). In the (a) and (b) panels, only the catalytic cysteine is shown in the structures of LcTS, hTS, MtbTS, and BsTS for clarity.
Molecules 24 01257 g007
Molecules 24 01257 g008 550
Figure 8. (a) Structural superimposition between the closed (white cartoon and carbon atoms; H-bonds as light grey dashed lines) and the open (dark grey cartoon and carbons) states of EfTS. (b) Structural comparison of the active (pink cartoon and carbon atoms, H-bonds as pink dashed lines) and the inactive (purple cartoon and carbon atoms, H-bonds as purple dashed lines) conformations of hTS.
Figure 8. (a) Structural superimposition between the closed (white cartoon and carbon atoms; H-bonds as light grey dashed lines) and the open (dark grey cartoon and carbons) states of EfTS. (b) Structural comparison of the active (pink cartoon and carbon atoms, H-bonds as pink dashed lines) and the inactive (purple cartoon and carbon atoms, H-bonds as purple dashed lines) conformations of hTS.
Molecules 24 01257 g008

Share and Cite

MDPI and ACS Style

Pozzi, C.; Ferrari, S.; Luciani, R.; Tassone, G.; Costi, M.P.; Mangani, S. Structural Comparison of Enterococcus faecalis and Human Thymidylate Synthase Complexes with the Substrate dUMP and Its Analogue FdUMP Provides Hints about Enzyme Conformational Variabilities. Molecules 2019, 24, 1257. https://doi.org/10.3390/molecules24071257

AMA Style

Pozzi C, Ferrari S, Luciani R, Tassone G, Costi MP, Mangani S. Structural Comparison of Enterococcus faecalis and Human Thymidylate Synthase Complexes with the Substrate dUMP and Its Analogue FdUMP Provides Hints about Enzyme Conformational Variabilities. Molecules. 2019; 24(7):1257. https://doi.org/10.3390/molecules24071257

Chicago/Turabian Style

Pozzi, Cecilia, Stefania Ferrari, Rosaria Luciani, Giusy Tassone, Maria Paola Costi, and Stefano Mangani. 2019. "Structural Comparison of Enterococcus faecalis and Human Thymidylate Synthase Complexes with the Substrate dUMP and Its Analogue FdUMP Provides Hints about Enzyme Conformational Variabilities" Molecules 24, no. 7: 1257. https://doi.org/10.3390/molecules24071257

APA Style

Pozzi, C., Ferrari, S., Luciani, R., Tassone, G., Costi, M. P., & Mangani, S. (2019). Structural Comparison of Enterococcus faecalis and Human Thymidylate Synthase Complexes with the Substrate dUMP and Its Analogue FdUMP Provides Hints about Enzyme Conformational Variabilities. Molecules, 24(7), 1257. https://doi.org/10.3390/molecules24071257

Article Metrics

Back to TopTop