Bacterial tRNA-guanine transglycosylase (Tgt) catalyses the exchange of the genetically encoded guanine at the wobble position of tRNAsHis,Tyr,Asp,Asn by the premodified base preQ1, which is further converted to queuine at the tRNA level. As eucaryotes are not able to synthesise queuine de novo but acquire it through their diet, eucaryotic Tgt directly inserts the hypermodified base into the wobble position of the tRNAs mentioned above. Bacterial Tgt is required for the efficient pathogenicity of Shigella sp, the causative agent of bacillary dysentery and, hence, it constitutes a putative target for the rational design of anti-Shigellosis compounds. Since mammalian Tgt is known to be indirectly essential to the conversion of phenylalanine to tyrosine, it is necessary to create substances which only inhibit bacterial but not eucaryotic Tgt. Therefore, it seems of utmost importance to study selectivity-determining features within both types of proteins. Homology models of Caenorhabditis elegans Tgt and human Tgt suggest that the replacement of Cys158 and Val233 in bacterial Tgt (Zymomonas mobilis Tgt numbering) by valine and accordingly glycine in eucaryotic Tgt largely accounts for the different substrate specificities. In the present study we have created mutated variants of Z. mobilis Tgt in order to investigate the impact of a Cys158Val and a Val233Gly exchange on catalytic activity and substrate specificity. Using enzyme kinetics and X-ray crystallography, we gained evidence that the Cys158Val mutation reduces the affinity to preQ1 while leaving the affinity to guanine unaffected. The Val233Gly exchange leads to an enlarged substrate binding pocket, that is necessary to accommodate queuine in a conformation compatible with the intermediately covalently bound tRNA molecule. Contrary to our expectations, we found that a priori queuine is recognised by the binding pocket of bacterial Tgt without, however, being used as a substrate.
Citation: Biela I, Tidten-Luksch N, Immekus F, Glinca S, Nguyen TXP, Gerber H-D, et al. (2013) Investigation of Specificity Determinants in Bacterial tRNA-Guanine Transglycosylase Reveals Queuine, the Substrate of Its Eucaryotic Counterpart, as Inhibitor. PLoS ONE 8(5): e64240. https://doi.org/10.1371/journal.pone.0064240
Editor: Lennart Randau, Max-Planck-Institute for Terrestrial Microbiology, Germany
Received: January 17, 2013; Accepted: April 9, 2013; Published: May 21, 2013
Copyright: © 2013 Biela et al. This is an open-access article distributed under the terms of the Creative Commons Attribution License, which permits unrestricted use, distribution, and reproduction in any medium, provided the original author and source are credited.
Funding: This work was supported by the Philipps-University of Marburg and the German Research Foundation (Graduiertenkolleg “Protein Function at the Atomic Level” and DFG grant KL1204/11-1). The travel costs to the BESSY II synchrotron in Berlin were covered by the Helmhotz-Zentrum Berlin. The funders had no role in study design, data collection and analysis, decision to publish, or preparation of the manuscript.
Competing interests: The authors have declared that no competing interests exist.
Transfer RNA–guanine transglycosylase (Tgt, EC 184.108.40.206) catalyses the exchange of a specific guanine base in tRNA molecules by a substituted 7-deazaguanine. Although Tgt is found in all three domains of life, the specificity of this enzyme with respect to (i) the tRNA substrate, (ii) the position of the guanine base therein to be exchanged, and (iii) the 7-deazaguanine derivative to be inserted differs in archaea, bacteria and eucaryotes (for review see ). Thus, the archaeal Tgt inserts preQ0 at position 15 of the majority of archaeal tRNAs where it is further converted to archaeine (for chemical formulae see Figure 1). Located at the “elbow” of the L-shaped tRNA the modification stabilises the overall tRNA structure by supporting the formation of the non-canonical Levitt base pair with cytosine 48 .
preQ0, 7-cyano-7-deazaguanine; preQ1, 7-aminomethyl-7-deazaguanine; queuine = 7-(((4,5-cis-dihydroxy-2-cyclopenten-1-yl) amino) methyl)-7-deazaguanine.
In contrast, both bacterial and eucaryotic Tgts are required for the introduction of the hypermodified base queuine into position 34 (the anticodon “wobble position”) of tRNAsHis,Tyr,Asp,Asn all of which have a uracil 33 – guanine 34 – uracil 35 sequence in common , . Although no distinct function for queuine has been demonstrated yet, its presence within the tRNA anticodon suggests that it may be involved in coordinating translational fidelity and speed.
Bacterial Tgt replaces the genetically encoded guanine at the above-mentioned position by the queuine-precursor preQ1. This premodified base is synthesised from guanosine 5′-triphosphate in a pathway employing GTP cyclohydrolase I (FolE) , 6-carboxy-5,6,7,8-tetrahydropterin synthase (QueD) , an S-adenosyl-l-methionine-dependent organic radical-generating enzyme (QueE), , preQ0 synthetase (QueC = ToyM)  and a nitrile reductase (QueF) –. Once incorporated into tRNA, preQ1 is further converted to the functional queuine in two consecutive steps catalysed by S-adenosylmethionine:tRNA ribosyltransferase-isomerase (QueA) – and the coenzyme B12-dependent epoxyqueuosine reductase (QueG) ,  (Figure 2).
Substrates and cosubstrates: GTP, guanosine 5′-triphosphate; AdoMet, S-adenosylmethionine; B12, coenzyme B12; preQ0, 7-cyano-7-deazaguanine; preQ1, 7-aminomethyl-7-deazaguanine; enzymes: FolE, GTP cyclohydrolase I; QueD, 6-carboxy-5,6,7,8-tetrahydropterin synthase; QueE, 7-carboxy-7-deazaguanine synthase; QueC, preQ0 synthetase; QueF, preQ0 reductase; Tgt, tRNA-guanine transglycosylase; QueA, S-adenosylmethionine:tRNA ribosyltransferase-isomerase; QueG, epoxyqueuosine reductase.
Bacterial Tgt functions as a homodimer in which the protomer consists of a (βα)8 barrel harbouring a Zn2+ binding subdomain close to the C-terminus . For sterical reasons, this dimer is, although endowed with two active sites, able to bind and convert only one substrate tRNA molecule at a time . The reaction catalysed by bacterial Tgt is accurately documented by numerous biochemical studies and crystal structures of Tgt from Zymomonas mobilis determined in its apo-form, in the presence of guanine, preQ1 or small molecule inhibitors and in complex with an RNA substrate , –. The reaction follows a ping-pong mechanism including a covalent Tgt⋅tRNA intermediate (Figure 3).
(A and B) The glycosidic bond of guanosine 34 is cleaved via nucleophilic attack by the Asp280 carboxylate resulting in the formation of a covalent Tgt⋅tRNA intermediate. (C and D) Guanine is replaced by preQ1 which is incorporated into the tRNA via nucleophilic attack of the ribose 34 anomeric carbon by N9 of preQ1. Notably the replacement of guanine by preQ1 in the binding pocket of Tgt induces a flip of the Leu231/Ala232 peptide bond. The formation of a hydroxide and an oxonium ion as byproducts of the reaction is assumed to be responsible for its irreversibility as mutual neutralisation will efficiently detract these ions from equilibrium. H-bonds are indicated by dashed lines.
Since eucaryotes are, other than bacteria, not capable of synthesising queuine de novo but rather acquire this modified base from their diet or from the gut flora, eucaryotic Tgt has to directly recognise and insert queuine into position 34 of tRNAsHis,Tyr,Asp,Asn. This stands in contrast to bacterial Tgt which was reported to be unable to accept this base as a substrate , . Unlike its bacterial counterpart, eucaryotic Tgt constitutes a heterodimer with both subunits, however, being homologous to the bacterial protomer , . Accordingly, both subunits contain the three cysteines as well as the histidine required for the coordination of the structural Zn2+ ion. However, only one subunit includes the residues known to be important for catalysis, among these is the active-site nucleophile, Asp280 (Z. mobilis Tgt numbering) , . Obviously, eucaryotic Tgt consists of a catalytic subunit and a second subunit which most probably supports the binding and the orientation of the tRNA substrate during catalysis.
It was shown that a functional Tgt is required for efficient pathogenicity of Shigella bacteria which are the causative agents of bacillary dysentery. A null-mutation in the tgt gene leads to a strongly reduced translation of virF-mRNA encoding a transcriptional activator required for the expression of a large number of Shigella pathogenicity genes . So far, the exact reason for this phenomenon is unknown, though Hurt et al. showed that Tgt is able to replace guanine 421 of virF mRNA by preQ1 . This unusual modification of an mRNA molecule might possibly have a stimulating effect on its translation. In any case, the fact that full pathogenicity of Shigella sp. relies on Tgt activity encouraged us to use this enzyme as a target for the rational design of anti-Shigellosis compounds. Meanwhile, based on the high-resolution crystal structure of Z. mobilis Tgt, inhibitors which show an affinity to bacterial Tgt down to the single-digit nanomolar range have been synthesised –.
Since a Tgt enzyme is present in humans as well, it is highly desirable to create inhibitors which preferably bind the bacterial enzyme while leaving the eucaryotic one unaffected. This seems of particular significance as recent studies performed on mice showed that a queuine deficiency or disruption of the tgt gene impairs the conversion of phenylalanine to tyrosine due to uncontrolled oxidation of the cofactor tetrahydrobiopterin . Bearing this observation in mind, it is of utmost importance to study selectivity-determining features within both types of proteins.
Although no crystal structure of a eucaryotic Tgt has been determined yet, a homology model of the Caenorhabditis elegans Tgt catalytic subunit that is based on the structure of Z. mobilis Tgt as a template, suggests a large structural similarity of the active sites of both bacterial and eucaryotic Tgt . However, in the eucaryotic enzyme, the recognition of the bulkier substrate is most probably enabled by a spatial expansion of the binding pocket. The enlargement of the binding pocket is caused by a single replacement of Val233 (Z. mobilis Tgt numbering) in bacterial Tgt by glycine in the eucaryotic catalytic subunit. Apart from that, the model suggests that only minor changes might be necessary in order to convert the binding pocket of bacterial Tgt such that it exhibits the specificity of the eucaryotic enzyme. Hence, in an attempt to generate a model system for the active site of human Tgt and to gain insights into the relevance of particular amino acids for substrate base selectivity, we adapted the Z. mobilis Tgt active site by site-directed mutagenesis in order to mimic that of the human enzyme. This paper describes the extensive analysis of mutated Z. mobilis Tgt variants created with this objective.
Generation of an in silico homology model of the human Tgt catalytic subunit
In 2009 Boland et al. reported the first successful isolation and characterisation of an enzymatically active eucaryotic Tgt, which was the heterologously produced heterodimeric murine enzyme . Shortly after that, Chen et al. published the production, purification and kinetic characterisation of recombinant human Tgt . However, no crystal structure of either of these enzymes is available yet, and the only structural information concerning the active site of a eucaryotic Tgt originates from a homology model of the Caenorhabditis elegans catalytic subunit . As the complete sequence of the human catalytic subunit has meanwhile become available ,  we created a model of this orthologue using the crystal structure of Z. mobilis Tgt as a template (for experimental details see the “Materials and Methods” section). The model indicates that most residues establishing the active centre and substrate binding pocket in the bacterial and human enzyme are identical. A significant difference, however, is the exchange of Val233 in Z. mobilis Tgt by a glycine (Gly232) in human Tgt (Figure 4). The exchange leads to an enlarged binding pocket of the human enzyme, being vital to accommodate the dihydroxy-cyclopentenyl side chain of queuine which is missing in preQ1, the physiological substrate of the bacterial enzyme (Figure 1). A further conspicuous difference which might influence substrate selectivity is the exchange of Cys158 in Z. mobilis Tgt by a valine residue (Val161) in human Tgt. The side chain of Val161 in the model of human Tgt is at a position where it is likely to come in contact with the dihydroxy-cyclopentenyl moiety of a bound queuine molecule. Lastly, there is a conservative amino acid exchange within the binding pocket of the human compared to the Z. mobilis enzyme which will, however, most probably not affect substrate selectivity. Tyr106 within the active centre of Z. mobilis Tgt forms via its aromatic side chain a stacking interaction with the bound substrate base (see Figure 4). Not only in the human enzyme it is replaced by a phenylalanine (Phe109), but also in the majority of bacterial Tgts whose sequences are known so far. It must be noted that all of the mentioned amino acid exchanges can be observed in the model of the C. elegans Tgt catalytic subunit as well .
A) Detail of Z. mobilis Tgt·preQ1 complex crystal structure (PDB-code: 1p0e) showing the active site with the bound substrate in stick representation. Carbon atoms of protein residues are coloured in green, those of preQ1 in orange. B) Homology model of human Tgt created with the Z. mobilis Tgt crystal structure as a template. The close up shows active site residues (carbon atoms in grey) superimposed with preQ1 (carbon atoms in orange) as present in 1p0e. The coordinates of the homology model are provided within the Supporting Information (Coordinates S1).
Point mutations aimed at enabling Z. mobilis Tgt to bind queuine and kinetic characterisation of the mutated variants
In order to investigate the importance of Gly232 and Val161 in human Tgt for queuine recognition, we created a doubly mutated variant of the Z. mobilis enzyme in which the corresponding Val233 and Cys158 were exchanged by glycine and valine, respectively. In addition, we created two further variants, each containing solely one of the above-mentioned amino acid exchanges. To resemble the situation in the active site of human Tgt, we did not introduce the mutations into wild type Z. mobilis Tgt but into the Tyr106Phe variant of Z. mobilis Tgt. This variant had been created in the course of a former study and it had been shown that the mutation of Tyr106 to phenylalanine has no measurable impact on any of the catalytic properties of the enzyme . In the following, this mutation will not be mentioned explicitly anymore and Tgt(Tyr106Phe) will henceforth be referred to as “wild type” Tgt.
To analyse the influence the introduced Val233Gly and Cys158Val mutations have on the binding of the different substrate bases and on catalysis, we measured kinetic parameters for the mutated variants and “wild type” Tgt. At first, KM and kcat for guanine and tRNATyr were analysed via monitoring the incorporation of [8-3H]-guanine into tRNATyr. None of the mutations had, either alone or in combination, any significant influence on KM(guanine) or KM(tRNATyr), yet kcat had, compared to “wild type” enzyme, decreased for all three variants (see Table 1). While for Tgt(Cys158Val) the turnover number was only marginally reduced by a factor of two it was lowered by one order of magnitude for Tgt(Val233Gly). In Tgt(Cys158Val/Val233Gly) the combination of both mutations led to a decrease in kcat by two orders of magnitude.
Subsequently, kinetic parameters were determined for preQ1 by measuring the incorporation of [3H]-preQ1 into tRNATyr. For Tgt(Cys158Val) also kcat(preQ1) was only slightly reduced by a factor of three compared to “wild type” Tgt. Remarkably, however, this mutation sparked an increase of KM(preQ1) by one order of magnitude, a loss of affinity which had not been observed for guanine. In contrast, no decrease in preQ1 affinity was detected for Tgt(Val233Gly) while, compared to “wild type” Tgt, kcat(preQ1) had decreased by one order of magnitude. As observed during the use of guanine as a substrate, the combination of both mutations in Tgt(Cys158Val/Val233Gly) led to a decrease in kcat(preQ1) by two orders of magnitude. Furthermore, KM(preQ1) of Tgt(Cys158Val/Val233Gly) had increased by more than a factor of ten, confirming that the Cys158Val exchange results in a measurable loss of affinity to this substrate base.
Ultimately, we intended to determine kinetic parameters for the three mutated Tgt variants as well as for “wild type” Tgt with respect to queuine. Seemingly, low activity was observed with “wild type” Tgt, Tgt(Cys158Val) and Tgt(Val233Gly) by measuring the incorporation of [3H]-queuine into tRNATyr. Thorough analysis of the measured progress curves, however, revealed that the observed activities were obviously not due to the insertion of queuine into substrate tRNA. At queuine concentrations equal to or exceeding the concentration of tRNATyr (15 µmol·L−1), the initially observed insertion of the radiolabelled base into tRNA already came to a halt when <10% of the tRNA was labelled (data not shown). This observation may be interpreted such that the used [3H]-queuine preparation contained a [3H]-labelled contaminant which was inserted with a measurable turnover (this contaminant might possibly be 7-deaza-7-hydroxymethylguanine, resulting from the reduction of the corresponding aldehyde which was used as starting material for queuine synthesis ). After the majority of this more potent impurity was incorporated into tRNATyr, queuine was barely or not inserted at all. Accordingly, this unexpected restriction did not allow us to figure out whether “wild type” Tgt, Tgt(Cys158Val) and Tgt(Val233Gly) were indeed able to accept queuine as a substrate nor did it allow us to determine Michaelis-Menten parameters as an indicator for affinity and catalytic activity. Therefore, we applied an alternative assay tracing the decrease in radioactivity of tRNATyr labelled at position 34 with [8-3H]-guanine due to the incorporation of unlabelled queuine. Compared to the commercially purchased [3H]-queuine, the “cold” queuine used for this assay was produced via a completely different synthetic route with preQ1 as a starting material. NMR analysis of this queuine preparation had revealed no detectable preQ1 contamination implying that, if present, its portion amounted to <1‰ . In fact, when queuine was used from this highly pure preparation at a concentration of 50 µmol·L−1 no insertion of queuine into tRNATyr was observed for “wild type” Tgt or any of the mutated variants during a time period of four hours. In contrast, when, as a positive control, 10 µmol·L−1 (“cold”) preQ1 was used in this assay, insertion of this base into 90% of the tRNA (in this assay present at a concentration of 8 µmol·L−1) was achieved by “wild type” Tgt within <10 minutes (data not shown).
Affinity of tRNATyr to Tgt as determined by microscale thermophoresis
Since none of the Tgt variants investigated in this study showed turnover when queuine was used as a substrate it was not possible to determine KM(queuine) as a measure of affinity. Therefore, in order to gain information about the ability of these variants to bind queuine we intended to use “microscale thermophoresis” to quantify dissociation constants (KD) of the enzyme·queuine complexes. This method is based on a microscale temperature gradient which is produced in a solution within a capillary by an infrared LED laser. Proteins (as well as any other molecules) show a directional motion along the temperature gradient determined by their size, charge and hydration shell which in turn are influenced by the presence or absence of a bound ligand. Any change in the above-named parameters caused by ligand binding affects the thermophoretic movement of the investigated protein, allowing the determination of binding affinities . To assess the applicability of this method to Z. mobilis Tgt we intended to determine KD values for guanine, preQ1, queuine and tRNATyr complexes of Tgt. However, no change in thermophoresis was observed upon addition of guanine, preQ1 and queuine proving this method to be unsuitable to investigate the affinities of these bases to Tgt and its mutated variants.
In contrast, a strong influence on the thermophoretic behaviour of Tgt was noticed upon binding of the macromolecular substrate tRNATyr enabling the determination of KD(Tgt·tRNATyr) which amounted to 36.2 nmol·L−1±5.7 nmol·L−1 (Figure 5). This value is considerably lower than KM(tRNATyr) (Table 1) indicating an affinity of Tgt to this substrate which is clearly higher than so far assessed by enzyme kinetics studies. The reason for this discrepancy may be that the binding of guanine to apo-Tgt prevents the binding of tRNATyr to the enzyme. Thus, guanine not only acts as a substrate but also as a competitive inhibitor with respect to tRNA. As guanine is present in a saturating concentration in any assay that aims at determining KM(tRNATyr) of Tgt, the recorded value may not constitute a reliable measure but will rather lead to a significant underestimation of the enzyme's affinity to tRNATyr.
Alexa Fluor®647 labelled Tgt at a concentration of 50 nmol·L−1 was incubated with varying amounts of tRNATyr. The difference in normalised fluorescence as a measure of change in thermophoresis is plotted against the concentration of tRNATyr.
Inhibition of Tgt and its mutated variants by queuine
Since queuine is not used as a substrate by “wild type” Tgt and our mutated variants, any specific binding of this base to the active centres of these enzymes should inevitably cause their inhibition. To verify an inhibitory effect of queuine on Tgt activity, we measured the activity of “wild type” Tgt, Tgt(Cys158Val), Tgt(Val233Gly) and Tgt(Cys158Val/Val233Gly) using guanine and tRNATyr as substrates both in the presence and absence of a low µmol·L−1 concentration of queuine. Indeed, a considerable decrease in acitivity dependent on queuine was observed for all investigated Tgt variants (see below).
As inhibitors mimicking the nucleobases guanine or preQ1 are basically able to inhibit Tgt in two different ways, we next determined the inhibition mode via that queuine acts on the investigated enzyme variants. If an inhibitor binds to the guanine 34/preQ1 34 subpocket of the apo-enzyme, it will inhibit the tRNA from accessing the enzyme and thus it will act as a competitive inhibitor with respect to the tRNA substrate. If, however, such an inhibitor occupies this subpocket after tRNA binding and the removal of guanine 34 it will prevent the substrate base preQ1 from binding. Accordingly, any further reaction of the covalent Tgt·tRNA intermediate is disabled which corresponds to an uncompetitive inhibition with respect to the tRNA substrate. Nucleobase mimetics of comparable size as guanine or preQ1 normally act via both inhibition modes. Nucleobase mimetics endowed with bulky exocyclic substituents, however, generally constitute purely competitive inhibitors with respect to tRNA as their binding to the covalent Tgt·tRNA complex would sterically interfere with the tRNA sugar phosphate backbone.
To figure out the inhibition mode via that queuine acts on the investigated Tgt variants we applied a trapping experiment which had been used for a similar purpose by Meyer et al. . Incubation of Tgt with substrate tRNA in the presence of an uncompetitive inhibitor in excess leads to a considerable stabilisation of the covalent Tgt·tRNA intermediate which can be visualised in terms of two retarded bands on a Coomassie-stained gel after SDS-PAGE of the reaction mixture (the presence of two retarded bands representing this complex results from different tRNA conformers present under the applied PAGE conditions ). In the absence of any inhibitor, only a very small amount of the covalent intermediate is detectable under the used assay conditions. The presence of excess inhibitor which solely and efficiently acts as a competitive inhibitor with respect to substrate tRNA entirely suppresses the formation of the covalent intermediate.
Thus, we incubated “wild type” Tgt, Tgt(Cys158Val), Tgt(Val233Gly) and Tgt(Cys158Val/Val233Gly) with tRNATyr in the presence of excess queuine. As a control, we incubated each of these Tgt variants solely with tRNATyr as well as with tRNATyr plus an excess of the preQ1 mimetic 2,6-diamino-3H-quinazolin-4-one (DAQ) (Figure 6A) which constitutes a potent uncompetitive inhibitor of Tgt (Kiu = 0.6 µmol·L−1) . Subsequently, we subjected the reaction mixtures to SDS-PAGE. In the case of “wild type” Tgt and Tgt(Cys158Val) no retarded band representing the covalent Tgt·tRNA intermediate was detectable on the Coomassie-stained gel, when, in addition to the enzyme, only tRNATyr was present in the reaction mixture (Figure 6B, lanes 2 and 8). This indicates that any excised guanine was quickly reinserted into tRNA keeping the amount of the covalent complex below the detection limit of the assay. In contrast, under the same conditions a faint band representing the covalent enzyme·tRNA complex was observed for Tgt(Val233Gly) and Tgt(Cys158Val/Val233Gly) indicating that the reinsertion rate of the excised guanine was significantly decreased with these Tgt variants (Figure 6B, lanes 5 and 11). When, in addition to tRNATyr excess DAQ was added, in the case of all Tgt variants the majority of the enzyme was trapped in a covalent complex formed with tRNATyr. On the Coomassie-stained gel this complex was visible as two clear retarded bands concomitant with considerable weakening of the band corresponding to the uncomplexed enzyme (Figure 6B, lanes 4, 7, 10 and 13). When queuine, instead of DAQ, was added to the reaction mixture, the formation of the covalent intermediate was completely suppressed in the case of “wild type” Tgt, Tgt(Cys158Val) and Tgt(Val233Gly) (Figure 6B, lanes 3, 6 and 9). This suggests that for these Tgt variants, queuine predominantly acts as a competitive inhibitor with respect to substrate tRNA. Solely in the case of Tgt(Cys158Val/Val233Gly) a very faint band representing the covalent enzyme·tRNA complex was visible in the presence of excess queuine (Figure 6B, lane 12). This may indicate that, in the case of this mutated variant, queuine is to some extent able to bind to the guanine 34/preQ1 subpocket of the covalent enzyme·tRNA complex resulting in an inhibition uncompetitive with tRNA binding. The fact, however, that the band representing the covalent enzyme·tRNA complex is clearly weaker than that observed in the absence of queuine suggests that queuine will also mainly bind to this mutated variant when present in the apo-form.
A) Chemical structure of 2,6-diamino-3H-quinazolin-4-one (DAQ), an uncompetitive inhibitor of Tgt. B) SDS-PAGE analysis of reaction mixtures of Tgt or mutated variants thereof and tRNATyr under conditions indicated. SM, size marker; q, queuine. While DAQ causes retarded Tgt bands by stabilising the covalent Tgt·tRNA intermediate, queuine lacks this ability for most of the investigated Tgt variants. Solely in case of Tgt(Cys159Val/Val233Gly) a faint retarded band is visible indicating that queuine may to some extent be able to bind to the guanine 34/preQ1 subpocket of the covalent enzyme·tRNA complex.
To gain information concerning the affinity of queuine to “wild type” Tgt and the mutated variants we determined, according to the method described in , the corresponding competitive inhibition constants, with respect to tRNA (Kic), of queuine. Kic(queuine) amounted to 3.8 µmol·L−1±0.6 µmol·L−1 for “wild type” Tgt, 3.8 µmol·L−1±0.5 µmol·L−1 for Tgt(Cys158Val), 3.1 µmol·L−1±0.2 µmol·L−1 for Tgt(Val233Gly) and 8.9 µmol·L−1±1.2 µmol·L−1 for Tgt(Cys158Val/Val233Gly). These results show that all studied Tgt variants including “wild type” Tgt are able to bind queuine with nearly identical affinity.
Crystal structure analyses of “wild type” Tgt and its mutated variants
To allow the interpretation of the obtained data at a structural level, we determined the crystal structures of the mutated Tgt variants created in this study in their apo-forms as well as in complex with preQ1 and queuine. In addition, we determined the crystal structure of “wild type” Tgt with a bound queuine molecule. Structures of “wild type” Tgt in its apo-form and in complex with preQ1 had already been published in a former study  and thus, were available in the protein data bank (PDB codes: 1ozm and 1ozq, respectively). An overview of the crystal structures considered in the present study is given in Table S1, while detailed data statistics are presented in Tables 2, 3 and 4.
The 2|Fo|-|Fc| electron density maps of all apo-structures clearly allow the identification of the introduced mutations, although a rather poorly defined density is present for Gly233 in both the structures of Tgt(Val233Gly) and Tgt(Cys158Val/Val233Gly). In the electron density maps of Tgt(Cys158Val) and of Tgt(Cys158Val/Val233Gly) the isopropyl side chain of Val158 is excellently defined. This is contrary to the sulfanylmethyl group of the original Cys158 whose side chain is, obviously due to its flexibility, poorly defined in the electron density maps of virtually all Z. mobilis Tgt crystal structures determined so far. Superimposition of the apo-structures of the mutated variants and “wild type” Tgt revealed that none of the amino acid exchanges implicates any significant structural change concerning the remaining part of the protein (mean rmsd 0.23 Å±0.02 Å).
Next, we analysed and compared the structures of the studied Tgt variants in complex with preQ1. In all preQ1-bound structures the ligand appears well-defined in the respective electron density map. Superimposition of the structural models reveals that preQ1 is identically positioned in all investigated variants including “wild type” Tgt (mean rmsd = 0.20 Å±0.07 Å). Furthermore, no differences were observed with respect to the catalytic Asp280 and the conformations of amino acids known to form direct interactions with the bound preQ1 ligand. The most conspicuous differences among the preQ1-bound structures concern a small cavity separating the side chains of amino acid residues 158 and 233 (Figure 7). In “wild type” Tgt this cavity harbors two well-ordered water molecules (Figure 7A) which are displaced in the Tgt(Cys158Val)·preQ1 complex structure by the isopropyl side chain of Val158 (Figure 7C). In the structure of preQ1-bound Tgt(Val233Gly) this cavity is substantially widened but harbors only one well-ordered water molecule. In addition, the electron density assigned to the preQ1 ligand does obviously not reflect the excellent resolution of this structure (1.19 Å) (Figures 7E and 8E). This is also indicated by the mean B-factor of preQ1 which is, in this structure, considerably elevated compared to the mean B-factor of the protein (33.0 Å2 versus 18.6 Å2). In contrast, in the structures of all other preQ1-bound Tgt variants the mean B-factor of preQ1 deviates only slightly from the mean B-factor of the protein (see Tables 2 and 4). The structure of preQ1-bound Tgt(Cys158Val/Val233Gly) reveals that, compared to Tgt(Val233Gly), the replacement of the hydrophilic and flexible sulfanylmethyl moiety of Cys158 by the hydrophobic isopropyl of valine leads to a regeneration of the original order in the substrate base binding pocket. The mean B-factor of the bound preQ1, which is excellently defined in the electron density map, hardly differs from the mean B-factor of the protein (15.7 Å2 versus 14.2 Å2). Furthermore, an arrangement of three highly ordered water molecules is present within the spacious cavity between Val158 and Gly233 (Figure 7G).
The solvent accessible surfaces of active sites from Z. mobilis Tgt variants are shown in bright yellow. The respective Tgt variant plus the bound ligand (shown in stick representation) are indicated in each sub-figure. Also amino acid residues at positions 158 and 233 are shown in stick representation. Carbon atoms of original amino acids and of the bound ligand are coloured green, those of mutated amino acids magenta. As the electron density assignable to the dihydroxy-cyclopentenyl moiety of queuine is poorly defined in all structures containing this ligand the coordinates of this moiety are not present in the respective structures deposited with the Protein Data Base. Accordingly, the conformations of the dihydroxy-cyclopentenyl shown in (D), (F) and (H) are tentative. To indicate this fact, the carbon atoms of this moiety are shown in grey. Selected water molecules are shown as red spheres. 2|Fo|-|Fc| (at σ 1.0) electron density is shown for the bound ligand and water molecules. 2|Fo|-|Fc| electron density contoured at a σ level of 1.0 is coloured blue, |Fo|-|Fc| electron density contoured at a σ level of 2.5 is coloured magenta. An overview of the crystal structures analysed in this study including resolutions and PDB codes is given in Table S1.
The respective Tgt variant plus the bound ligand are indicated in each sub-figure. Carbon atoms of original amino acids are coloured green, those of mutated amino acids as well as of the bound ligand orange. As the electron density assignable to the dihydroxy-cyclopentenyl moiety of queuine is poorly defined in all structures containing this ligand the coordinates of this moiety are not present in the respective structures deposited with the Protein Data Base. Accordingly, the conformations of the dihydroxy-cyclopentenyl shown in (D), (F) and (H) are tentative. To indicate this fact, the carbon atoms of this moiety are shown in grey. Selected water molecules are shown as red spheres. Electron density is shown for amino acid residues at positions 158 and 233 as well as for the ligand and for water molecules. The 2|Fo|-|Fc| electron density map contoured at a σ level of 1.0 is coloured blue. The green density represents an |Fo|-|Fc| omit map contoured at 2.5 σ. An overview of the crystal structures analysed in this study including nominal resolutions and PDB codes is given in Table S1.
A conspicuous structural change upon binding of preQ1 is observed within the binding pockets of those Tgt variants which harbour the Cys158Val mutation. Both in Tgt(Cys158Val) and Tgt(Cys158Val/Val233Gly) the binding of preQ1 provokes a shift of Val158 towards the ligand enabling five Van-der-Waals interactions of its isopropyl side chain with the 7-deazaguanine scaffold of preQ1 (3.5 Å to 4.3 Å calculated by CONTACSYM ). In addition, a noticeable change of the proximate Thr159 whose side chain is rotated by about 90° is observed (Figure 9A). So far, in no other crystal structure of Z. mobilis Tgt or any variant thereof such a conformational change of Thr159 has been observed upon ligand binding. To obtain indication of whether the reduced affinity of Tgt(Cys158Val) and Tgt(Cys158Val/Val233Gly) towards preQ1 arises from the described structural changes, we determined the crystal structure of Tgt(Cys158Val) in complex with guanine. If the observed conformational rearrangements actually account for the decrease in affinity to preQ1 we expected them to not occur upon guanine binding since the Cys158Val exchange has no measurable impact on guanine recognition. The crystal structure of the Tgt(Cys158Val)·guanine complex reveals that upon guanine binding the side chain of Val158 becomes largely disordered as it is ill-defined in the electron density map. The position of the main chain atoms of Val158 indicates that there is hardly any shift of this residue towards the ligand. Strikingly, no change of the Thr159 side chain conformation which closely resembles that of the apo-structure is observed (Figure 9B). We would like to note that binding of guanine in Tgt(Cys158Val), as in wild type Tgt, leads to a Leu231/Ala232 peptide bond conformation which is flipped compared to the preQ1-bound situation . In the preQ1-bound enzyme the carbonyl group of this peptide bond is exposed to the binding pocket while the backward-oriented amide forms an H bond to the deprotonated side chain carboxyl of Glu235. In contrast, upon guanine binding the NH-group of this peptide bond is exposed, while the backward-oriented carbonyl oxygen interacts with the protonated Glu235 side chain carboxyl group (see also Figure 3).
Carbon atoms of the Tgt(Cys158Val)·preQ1 complex are coloured pink in all sub-figures. (A) Superimposition (based on cα) of preQ1-bound Tgt(Cys158Val) and apo-Tgt(Cys158Val). Carbon atoms of apo-Tgt(Cys158Val) are coloured blue. Binding of preQ1 to Tgt(Cys158Val) provokes a shift of Val158 towards the ligand leading to the displacement of two water molecules (W1 and W2; shown as red spheres) which are present within this region in apo-Tgt(Cys158Val) and absent in the complex structure. In addition, the side chain of the proximate Thr159 rotates by about 90°. Exactly the same structural changes upon binding of preQ1 are observed for Tgt(Cys158Val/Val233Gly). (B) Superimposition (based on cα) of preQ1-bound Tgt(Cys158Val) and guanine-bound Tgt(Cys158Val). Carbon atoms of the Tgt(Cys158Val)·guanine complex are coloured yellow. In the Tgt(Cys158Val)·guanine complex, the side chain of Val158 becomes largely disordered. The Thr159 side chain adopts a similar conformation as observed in the apo-structure. (C) Superimposition (based on cα) of preQ1-bound Tgt(Cys158Val) and queuine-bound Tgt(Cys158Val). Carbon atoms of the Tgt(Cys158Val)·queuine complex are shown in grey. Binding of queuine obviously leads to disordering of the Val158 side chain as no electron density attributable to this isopropyl moiety is present in the electron density map of the refined Tgt(Cys158Val)·queuine complex structure. Also upon binding of queuine no conformational change of the Thr159 side chain is observed. It adopts a similar conformation as in the apo- and guanine-bound structures.
Ultimately, we determined the crystal structures of the studied Tgt variants in complex with queuine. Although electron density which can be attributed to a bound ligand is clearly present in the binding pocket of the refined structure of “wild type” Tgt crystallised in the presence of queuine it turned out to be too ill-defined to allow a definite placement of queuine in the model (Figures 7B and 8B). In contrast, the electron density map of the Tgt(Cys158Val)·queuine complex structure allowed the placement of the 7-deazaguanine scaffold and the exocyclic aminomethyl group of queuine. Clearly, this part of the ligand shows, as expected, a binding mode which strongly resembles that of preQ1 (Figures 7D and 8D). Only rudimentary density, however, is visible for the dihydroxy-cyclopentenyl moiety of queuine probably due to its enhanced residual mobility. Yet, the position of the aminomethyl group implicates the dihydroxy-cyclopentenyl pointing towards the uracil 33 nucleotide subpocket of the enzyme. This leads, compared to the preQ1-bound situation, to the displacement of a water molecule which forms an H bond to the exocyclic amino group of preQ1. This water is strictly conserved in the preQ1 complex structures of all investigated Tgt variants and designated “W” in Figures 8A, 8C, 8E and 8G. Superimposition of the queuine-bound Tgt(Cys158Val) structure with the structure of Tgt in complex with RNA  reveals that in the present conformation the dihydroxy-cyclopentenyl moiety of queuine sterically interferes with the ribose of the uracil 33 nucleotide and the phosphate at position 34. Hence, the binding of queuine in the observed conformation is obviously not compatible with the binding of a tRNA substrate. Notably, as observed for guanine, the presence of queuine in the substrate pocket of Tgt(Cys158Val) apparently completely disorders the Val158 side chain as there is no electron density assignable to this isopropyl moiety (Figure 8D). In contrast, this side chain is excellently defined in the electron density maps of apo- and preQ1-bound Tgt(Cys158Val) and Tgt(Cys158Val/Val233Gly). The positioning of the Val158 main chain atoms, however, suggests a significant shift of this residue towards the bound ligand although less pronounced as observed in the preQ1 complex structure of Tgt(Cys158Val). In accordance with the structure of the guanine-bound Tgt(Cys158Val), this shift is not concomitant with a rotation of the Thr159 side chain (Figure 9C).
Also the electron density maps of the Tgt(Val233Gly)·queuine and Tgt(Cys158Val/Val233Gly)·queuine complex structures enabled reliable placement of the 7-deazaguanine scaffold of the ligand which is, in both cases, similarly bound as in the Tgt(Cys158Val)·queuine complex. In both maps fragmentary density is visible for the dihydroxy-cyclopentenyl substituent (Figures 7F, 7H as well as 8F, 8H). Figures 7F and 7H show that the mutation of Val233 to glycine results in a considerable gain of space in the substrate binding pocket which allows the dihydroxy-cyclopentenyl of queuine to occupy the cavity located between Gly233 and the side chain of Cys/Val158. Within this cavity the dihydroxy-cyclopentenyl apparently has no specific interaction with the protein. As a consequence, it seems to be highly flexible which is reflected by the ill-defined electron density assigned to this moiety in both structures. As in the structure of queuine-bound Tgt(Cys158Val), nearly no electron density can be attributed to the side chain of Val158 in the Tgt(Cys158Val/Val233Gly)·queuine complex structure, indicating an increased mobility of this residue upon the binding of queuine. Also, in agreement with the structure of queuine-bound Tgt(Cys158Val), the positioning of the Val158 main chain atoms suggests a shift of this residue towards the ligand which is not concomitant with a rotation of the Thr159 side chain.
It must be noted that in the case of all queuine complex structures determined in this study the electron density assigned to the 7-deazaguanine scaffold of the ligand by far does not comply with the nominal resolution of the respective structure. Even in the case of the mutated variants where reliable placement of the scaffold into the binding pocket was possible the electron density within this area appears rather fuzzy or even patchy and lacks detail. It is likely that multiple conformations and the low occupancy (on average 60%) of queuine in the binding pocket provoked the poor electron density.
While eucaryotic Tgt exchanges the genetically encoded guanine by queuine at position 34 of tRNAsHis,Tyr,Asp,Asn, bacterial Tgt is not able to insert the latter hypermodified base into these tRNAs. Instead, it uses the queuine-precursor preQ1 as a substrate which is then further converted to the final queuine at the tRNA level. A homology model of the C. elegans Tgt catalytic subunit suggests that the exchange of Cys158 and Val233 in bacterial Tgt (Z. mobilis Tgt numbering) by valine and glycine, respectively, in eucaryotic Tgt largely accounts for the difference in substrate specificity between the Tgt enzymes of both domains of life . This assumption was supported by a homology model of the human Tgt catalytic subunit created in the present study. The replacement of Val233 by glycine results in a considerable gain of space in the substrate binding pocket most probably required for the accommodation of the dihydroxy-cyclopentenyl moiety of queuine. The side chain of the valine residue corresponding to Cys158 of Z. mobilis Tgt appears at a position where it might form an interaction with the dihydroxy-cyclopentenyl substituent. While Cys158 and Val233 are highly conserved in bacterial Tgt, the corresponding valine and glycine residues are invariant in all eucaryotic Tgt catalytic subunits whose sequences have been determined so far .
Based on the homology models of the C. elegans and human Tgt catalytic subunits, we replaced, via site-directed mutagenesis, Val233 and Cys158 in Z. mobilis Tgt by glycine and valine, respectively. In addition, to separately investigate the influence of these amino acid exchanges on substrate specificity and catalysis, we created two further variants, each containing solely one of the two mutations. However, the introduced changes which we desired for to convert substrate selectivity of bacterial towards eucaryotic Tgt did not result in an enzyme that is able to insert queuine into tRNA. Instead, the amino acid exchanges mainly interfere with catalysis by reducing kcat(guanine) and kcat(preQ1). While the reduction is not of great significance for Tgt(Cys158Val) (2- to 3-fold), it accounts for one order of magnitude for Tgt(Val233Gly) and for two for Tgt(Cys158Val/Val233Gly). The crystal structures of these Tgt variants, determined in complex with preQ1, clearly show that preQ1 is, in each case, identically positioned as in the wild type, ruling out a substrate misorientation with respect to any catalytically relevant residue. Instead, the mutated residues may exert influence on the properties of a nearby catalytic water molecule acting as a proton donor during guanine excision (Figures 3A and 3B).
A notable consequence of the Cys158Val exchange is the significantly decreased affinity of the enzyme towards preQ1 but not guanine. A similar phenomenon was reported by Chen et al.  who mutated the corresponding cysteine of E. coli Tgt to valine, resulting in a dramatical loss of affinity to preQ1. Consistently, a measurable gain in preQ1 affinity was observed by this group for the human enzyme upon mutation of the corresponding Val161 to cysteine. The study does, however, not provide any data demonstrating the impact of these mutations on guanine as a substrate. As already proposed by Chen et al. , it seems likely that, in eucaryotes, a valine at the mentioned position in the catalytic subunit of eucaryotic Tgt preferably prevents the (irreversible!) insertion of preQ1 into tRNA. Our data provide evidence that this is achieved without the loss of affinity towards guanine which, most likely, would result in an attenuated affinity to the unmodified substrate tRNAs comprising guanine at position 34.
The crystal structures of Tgt(Cys158Val) and Tgt(Cys158Val/Val233Gly), each in complex with preQ1, reveal, compared to the corresponding apo-forms, a shift of Val158 towards the ligand. This allows the isopropyl side chain of this residue to form Van-der-Waals contacts to the substrate. This structural change is concomitant with a ca. 90° rotation of the Thr159 side chain thus resulting in a novel conformation which has, until now, not been observed in any other crystal structure of Z. mobilis Tgt or a mutated variant thereof. The crystal structure of Tgt(Cys158Val) in complex with guanine reveals that there is no conformational change of Thr159 upon guanine binding. Obviously, the Thr159 conformational change is triggered by preQ1 and not by guanine. This observation is of greater remarkability as the Thr159 side chain remains at large distance without any direct contact to the aminomethyl group of preQ1. The Penultimate Rotamer Library published by Lovell et al.  reports three preferred rotamers for threonine observed with a relative frequency of 7%, 43%, and 49%. Notably, in the preQ1 complexes of Tgt(Cys158Val) and Tgt(Cys158Val/Val233Gly) Thr159 adopts the least populated conformer, which probably corresponds to the rotamer that is least energetically favourable. In contrast, the Thr159 side chain conformation observed in all other crystal structures of Z. mobilis Tgt matches with the rotamer found with a frequency of 43%. Accordingly, the side chain conformation of Thr159 induced upon preQ1 binding may well be correlated with the reduced preQ1 affinity observed upon mutation of Cys158 to valine. It should be noted, that Thr159 is in most eucaryotic Tgt catalytic subunits replaced by a nearly isosteric valine residue .
As neither Z. mobilis Tgt nor any of our mutated variants are able to use queuine as a substrate we investigated whether or not queuine is actually recognised by these enzymes. For that purpose, we tested if queuine was able to act as inhibitor of bacterial Tgt since its binding to the active site should inevitably prevent radiolabelled guanine from being inserted into tRNA. Indeed, a considerable inhibitory effect of queuine on Tgt activity was observed for all investigated enzyme variants including “wild type” Tgt. The recognition of queuine in the substrate binding pocket of “wild type” Tgt and Tgt(Cys158Val) seems surprising as these variants do not exhibit the space-opening Val233Gly exchange believed to be prerequisite for the accommodation of the dihydroxy-cyclopentenyl side chain of queuine. Trapping experiments revealed that queuine predominantly acts as a competitive inhibitor with respect to tRNA as a substrate on all studied Tgt variants. This means queuine binds to the respective apo-enzymes but hardly to the covalent enzyme·tRNA complexes formed upon the release of guanine. Solely in the case of Tgt(Cys158Val/Val233Gly), the variant that should best approach the eucaryotic enzyme, the result of the trapping experiment indicates that the covalent enzyme·tRNA complex may, though to a low extent, be able to bind queuine.
The crystal structure of Tgt(Cys158Val) in complex with queuine provides an evident explanation why this variant is able to bind queuine exclusively in its apo-form. The bulky side chain of Val233 does not prevent queuine from binding to the active site. Yet, it forces its dihydroxy-cyclopentenyl moiety into a position which is not compatible with tRNA binding due to clashes with the tRNA sugar phosphate backbone. The same is likely to be true for “wild type” Tgt although ill-defined electron density in this crystal structure does not allow a reliable placement of queuine into the substrate binding pocket of the refined model.
The crystal structures of Tgt(Val233Gly) and Tgt(Cys158Val/Val233Gly) with queuine reveal that the Val233Gly exchange allows the dihydroxy-cyclopentenyl substituent to occupy the created cavity between position 233 and 158. The adopted binding mode of queuine will not interfere sterically with the sugar-phosphate backbone of bound tRNA. Yet, the results of the trapping experiment suggest that Tgt(Val233Gly) is also not able to bind queuine after the formation of the covalent enzyme·tRNA complex. Tgt(Cys158Val/Val233Gly) is, if at all, only to a minor extent able to bind queuine after the formation of this complex. The fuzzy electron density corresponding to the bound queuine suggests high residual ligand flexibility accompanied by a significant disorder induced in the active sites of the studied Tgt variants. The latter becomes evident from elevated B-factors and ill-defined electron density of residues lining the substrate binding pocket. Possibly, the enhanced mobility of the substrate binding pocket and of the bound queuine in these complexes is not compatible with the constrictions induced by the formation of the covalent enzyme·tRNA complex. Anyway, the fact that queuine is not able to bind efficiently to the covalent complex of any Tgt variant provides a plausible explanation why it does not constitute a substrate. None of the crystal structures determined in this study nor the in silico model of the catalytic subunit of human Tgt provide any clue on how this problem is overcome by eucaryotic Tgt. Probably, further residues, that are more distant from the active centre but involved in positioning the tRNA substrate have to be changed as well to enable bacterial Tgt to insert queuine into tRNA. In addition, it has to be pointed out once more that eucaryotic Tgt not only consists of a catalytic subunit, which is closely related to the bacterial protomer but, in addition, also contains a second subunit, which is catalytically inactive. This second subunit might possibly be prerequisite to enable the enzyme to use queuine as a substrate by aligning the tRNA substrate in a manner that somehow compensates for the loss of activity observed in our mutated variants.
Comparison of the active centre of Z. mobilis Tgt with the modelled human Tgt catalytic subunit reveals that Ala232 adjacent to Val233 in the bacterial enzyme is replaced by a serine (Ser231) in human Tgt (Figure 4). This residue is involved in a peptide switch necessary to accommodate preQ1 after the excised guanine 34 left the binding pocket  (Figure 3). Although the main chain amide of Ala232 binds indirectly, via a water molecule, to N7 of guanine 34 its side chain methyl group forms no interaction with any substrate. As this residue is replaced by a serine in many bacterial Tgts too, it seems unlikely that it contributes to substrate specificity or catalytic activity. Nevertheless, we introduced the Ala232Ser mutation into Tgt(Cys158Val/Val233Gly) to investigate its impact. For comparison, the Ala232Ser mutation was also introduced into “wild type” Tgt. Kinetic measurements showed that the Ala232Ser conversion further reduced the catalytic activity of Tgt(Cys158Val/Ala232Ser/Val233Gly). The residual turnover observed for this variant with both guanine and preQ1 as substrates was too small to permit the determination of reliable Michaelis-Menten parameters, due to the low signal to noise ratio of the measured data. Interestingly, a pronounced 102-fold decrease in kcat compared to “wild type” Tgt was also observed for Tgt(Ala232Ser) using guanine or preQ1 as a substrate (data not shown). Therefore, the Ala232Ser variants of Tgt were not considered further in this study. In addition, crystal structures that were determined of Tgt(Cys158Val/Ala232Ser/Val233Gly) in its apo-form, in complex with preQ1 and in complex with queuine do not show any significant differences to the corresponding ones of Tgt(Cys158Val/Val233Gly) and, due to redundance, will not be discussed in detail (data statistics and PDB codes of these structures are provided in Table S2 of the Supporting Information). Nevertheless, it is worth mentioning that, in the Tgt(Cys158Val/Ala232Ser/Val233Gly)·preQ1 complex the above-mentioned side chain rotation of Thr159, thought to correlate with the Cys158Val mutation upon binding of preQ1, is also observed. This conformational change is not visible in the structure of this variant in complex with queuine.
Materials and Methods
The crystal structure of Z. mobilis Tgt (PDB code 1r5y chain A) was used as a template to create a model of the human Tgt catalytic subunit (UniProtKB/Swiss-Prot  accession code Q9BXR0). Using ClustalW 1.83  the corresponding sequences aligned with 42% identity. Based on the alignment, ten homology models for human Tgt were calculated with MODELLER 6a . As no significant differences were apparent, the model with the lowest MODELLER target function value (11,429.19) was selected as representative. The coordinates of the homology model are provided within the Supporting Information (Coordinates S1).
Cloning and Tgt preparation
Site-directed mutagenesis was performed using the QuickChange™ kit (Stratagene) following the vendor's protocol. The oligonucleotides listed in Table 5 were used to introduce the mutations into the Z. mobilis tgt(Tyr106Phe) expression plasmid pET9d-ZM-Y106F . Sequence analysis of the entire tgt gene (MWG Biotech, Ebersberg) confirmed in each case the presence of the desired mutation(s) as well as the absence of any further unwanted mutation. Subsequently, the mutated plasmids were transformed into E. coli BL21(DE3)/pLysS cells. These cells were used for the preparation of the mutated Tgt variants following the protocol of Romier et al. .
Preparation of Escherichia coli tRNATyr
Preparation of unmodified E. coli tRNATyr (ECY2)  via in vitro transcription was done using the RiboMAX™ Large Scale RNA Production System-T7 (Promega) according to the vendor's protocol. The concentration of tRNA was determinded via UV photometry (λ = 280 nm).
Preparation of preQ1 and queuine
Preparation of preQ1 and queuine was carried out according to .
Determination of kinetic parameters
Progress curves of Tgt activity using guanine and tRNATyr as substrates were measured by monitoring incorporation of radiolabelled guanine into tRNATyr. The reaction proceeded at 37°C in 75 µL solutions containing 150 nmol·L−1 (of monomer) Z. mobilis Tgt [300 nmol·L−1 in case of Tgt(Cys158Val/Val233Gly)] and variable concentrations of E. coli tRNATyr and guanine (7.5% [8-3H]-guanine; 12 Ci/mmol, Hartmann Analytic). The assay was performed in 200 mmol·L−1 HEPES buffer pH 7.3, 20 mmol·L−1 MgCl2, and 0.037% (v/v) Tween 20 (Roth). Reactions were started by adding tRNA and [8-3H]-guanine to the protein solution. To allow the protein solution to adjust to assay temperature it was pre-incubated at 37°C for 10 min prior to substrate addition. After the reactions were started, 15 µL aliquots were taken at intervals of 1 to 4 min. Aliquots were immediately transferred to Whatman GC-F glass microfiber filters (GE Healthcare) and quenched with 10% (w/v) trichloroacetic acid at 0°C for 15 min. Unbound guanine was washed from the filters in 7 min intervals twice with 5% (w/v) trichloroacetic acid and twice with technical grade ethanol. Filters were dried at 60°C for 45 min. 3H incorporated into tRNA was quantified using liquid scintillation counting. Results from the aliquots were used to calculate initial velocity using GraFit (V. 4.09; Erithacus Software Ltd., 1999).
Michaelis-Menten parameters for tRNA and guanine were determined separately in duplicate and average values were calculated. Kinetic parameters for guanine were measured using 15 µmol·L−1 tRNATyr and concentrations of [8-3H]-guanine varying in the range of 0.5–20 µmol·L−1. Kinetic parameters for tRNA were measured using 20 µmol·L−1 [8-3H]-guanine and tRNATyr concentrations varying in the range of 0.25–15 µmol·L−1. Initial velocities in “counts per min” were transferred to µmol·L−1·min−1 using a calibration constant derived from liquid scintillation counting of [8-3H]-guanine solutions with variable concentrations. Kinetic parameters were determined via double-reciprocal linearisation and linear regression using GraFit.
Michaelis-Menten parameters for preQ1 were determined in the same manner as for guanine but using radiolabelled preQ1 ([methylene-3H]-7-aminomethyl-7-deazaguanine = [3H]-preQ1; 7.0 Ci/mmol, Moravek Biochemicals Inc., California, USA) as substrate base. The concentration of preQ1 was varied between 0.5–15 µmol·L−1 for “wild type” Tgt and Tgt(Val233Gly) or rather 1–50 µmol·L−1 for Tgt(Cys158Val) and Tgt(Cys158Val/Val233Gly).
In the same manner, enzymatic activity was analysed using [3H]-queuine (7.0 Ci/mmol, Moravek Biochemicals Inc., California, USA) as substrate base at concentrations of up to 50 µmol·L−1. Alternatively, enzymatic activity with queuine as substrate base was measured via monitoring the removal of [8-3H]-guanine from tRNATyr radiolabelled in position 34 as described in  but with the substrate base preQ1 replaced by queuine. Radiolabelled tRNATyr was used in a concentration of 8 µmol·L−1. The concentration of queuine amounted to 50 µmol·L−1 for all inspected Tgt variants.
Determination of inhibition constants
Inhibition constants of queuine (competitive against tRNA) were determined for “wild type” Tgt and mutated variants as described in .
SDS-PAGE trapping experiment
5 µmol·L−1 Z. mobilis Tgt (monomer), 100 µmol·L−1 E. coli tRNATyr (ECY2) and, if necessary, 1 mmol·L−1 of queuine or rather 2,6-diamino-3H-quinazolin-4-one in 10 µL of 100 mmol·L−1 HEPES buffer, pH 7.3, 20 mmol·L−1 MgCl2, and 5 mmol·L−1 dithiothreitol were incubated for 1 h at 25°C. A total of 10 µL of SDS loading buffer [250 mmol·L−1 TrisHCl pH 6.8, 8% (w/v) SDS, 40% (v/v) Glycerol, 0.04% (w/v) bromophenol blue, 8% (v/v) 2-sulfanylethanol] was added and incubated for another hour at 25°C to allow proper unfolding. 10 µL of each sample were then loaded onto a 15% SDS polyacrylamide gel and electrophoresis was performed with SDS running buffer [25 mmol·L−1 TrisHCl pH 8.8, 200 mmol·L−1 glycine, 0.1% (w/v) SDS]. Gels were stained with Coomassie® brilliant blue R-250 (Bio-RAD).
Microscale thermophoresis measurements
Z. mobilis Tgt at a concentration of 10 µmol·L−1 was labelled with Alexa Fluor®647 succinimidyl ester at a concentration of 40 mg·L−1 at room temperature for 30 min in a 500 mmol·L−1 NaCl solution buffered with 50 mmol·L−1 HEPES pH 8.1 (molar dye ∶ protein ratio≈3 ∶ 1). Excessive unreacted Alexa Fluor®647 was removed with a NAP5 sephadex column (GE Healthcare) equilibrated with 2 mol·L−1 NaCl, 1 mmol·L−1 EDTA solution buffered with 10 mmol·L−1 TrisHCl pH 7.8. Photometry at 650 nm and 280 nm indicated a label ∶ protein ratio of 0.8. The Alexa Fluor®647-Tgt solution was adjusted to 100 nmol·L−1 with 100 mmol·L−1 HEPES pH 7.3 buffer containing 20 mmol·L−1 MgCl2 and 0.037% (v/v) (≡323 µmol·L−1) Tween 20 (Roth). The final solution contained NaCl at a concentration of approximately 300 mmol·L−1. The tRNATyr ligand was dissolved in the same buffer (free of NaCl) at a concentration of 10 µmol·L−1. A series of fifteen 1 ∶ 1 dilutions of tRNATyr solution ∶ buffer solution was prepared producing tRNATyr concentrations ranging from 305 pmol·L−1 to 10 µmol·L−1. For thermophoresis, each of these solutions was mixed with one volume of Alexa Fluor®647-Tgt solution resulting in a constant concentration of fluorescence labelled Tgt of 50 nmol·L−1 and tRNATyr concentrations ranging from 153 pmol·L−1 to 5 µmol·L−1. After 10 min incubation followed by centrifugation at 10 000× g for 10 min, approximately 2 µL of each solution were filled into Monolith NT Standard treated capillaries (NanoTemper Technologies GmbH). Thermophoresis (including temperature jump) was measured at room temperature for 10 s by means of a Monolith NT.015 instrument (NanoTemper Technologies GmbH), using 100% LED power and 60% infrared laser power. Data of three independent runs were averaged and analysed using Origin 7 (Origin Lab). Curve fitting and KD calculation was done using the program NanoTemper Analysis 1.2.009 (NanoTemper Technologies GmbH) based on the following equation :
T = thermophoresis signal
U = minimal signal (unbound protein)
B = maximal signal (protein saturated with ligand)
cp = concentration of labelled protein
ci = concentration of ligand
Crystallisation, data collection, and processing
Crystals of the investigated Tgt variants suitable for ligand soaking were grown via the hanging-drop vapour diffusion method. Droplets were prepared by mixing 1 µL of concentrated protein solution (12 to 15 mg·mL−1 in 2 mol·L−1 NaCl, 10 mmol·L−1 Tris/HCl pH 7.8, 1 mmol·L−1 EDTA, 1 mmol·L−1 DTT) with 1 µL reservoir solution (11% (w/v) PEG 8,000, 100 mmol·L−1 Tris/HCl, pH 8.5, 1 mmol·L−1 DTT, 10% (v/v) DMSO). Crystals grew within one week at 18°C in the presence of 1.0 mL of reservoir solution.
For cocrystallisation of Tgt(Cys158Val) with guanine, guanine·HCl was dissolved in DMSO and added to the crystallisation droplet to a final concentration of 5 mmol·L−1. As guanine is, under the above-named conditions, not soluble up to this concentration a substantial portion of the compound precipitated. Crystals grew within the guanine precipitate in two weeks. To allow cocrystallisation of the Tgt variants with Q the compound was dissolved in DMSO and added to the droplet to a final concentration of 20 mmol·L−1. Crystals of the Tgt variants complexed to preQ1 were produced by a soaking procedure. The compound was dissolved in DMSO and added to 2 µL of reservoir solution to a final concentration of 10 to 20 mmol·L−1. Finally, a single pre-grown Tgt crystal was transferred into the droplet which was sealed against 1.0 mL of reservoir solution and soaked for 30 min.
For data collection, crystals were cryoprotected using glycerol. The glycerol and PEG 8,000 concentrations of the reservoir buffers were increased stepwise by transferring the crystals to six different 2 µL cryodroplets each with 30-min incubation times while sealed against 1.0 mL of the same solution (glycerol concentrations (v/v): 5%→10%→15%→20%→25%→30%; and PEG 8,000 concentrations (w/v): 5.0%→6.3%→7.5%→8.0%→8.8%→9.8%, respectively). These droplets also contained the ligands at the same concentrations as the soaking and cocrystallisation solutions. The cryo-soaked crystals were flash-frozen in liquid nitrogen. Data sets (3bld, 4dg0, 4e2v, 4hvx, 4h7z, 4h6e, 4hsh, 4hqv, 4gcx and “WT”-Tgt·queuine) were collected at cryo conditions (−173°C≡100 K) at the BESSY II (Helmholz-Zentrum, Berlin, Germany) beamlines BL-14.1 (λ = 0.91841 Å) and BL-14.2 (λ = 0.91841 Å) and with CuKα radiation (λ = 1.5418 Å) using a Rigaku RU-300 rotating-anode generator at 50 kV and 90 mA equipped with Xenocs focussing optics and an R-AXIS IV detector. All crystals tested exhibited monoclinic symmetry in space group C2 containing one monomer per asymmetric unit with Matthews coefficients of 2.3–2.4. Data processing and scaling was performed using the HKL2000 package  except for structure 4h7z which was processed using iMOSFLM 1.0.6  and SCALA . For all refined structures unit cell dimensions for the crystals, data collection and processing statistics are given in Tables 2, 3 and 4.
Coordinates of the apo-Tgt crystal structure (PDB-code: 1pud in case of the structures 3bl3, 3bld, 3blo) or rather coordinates of Tgt in complex with 2-[(thiophen-2-ylmethyl)amino]-1,7-dihydro-8H-imidazo[4,5-g]quinazolin-8-one (PDB-code: 3gev in case of structures 4dg0, 4e2v, 4hvx, 4h7z, 4h6e, 4hsh, 4hqv, 4gcx and “WT”-Tgt·queuine) were slightly modified (deletion of water and ligand as well as coordinates at the sites of mutation) before applying for initial rigid-body refinement of the protein molecule followed by repeated cycles of conjugate gradient energy minimisation, simulated annealing and B-factor refinement using the CNS program package . Refinement at the later stages was performed with SHELXL  for structures 3bl3, 3bld, and 3blo. Here, up to 50 cycles of conjugate gradient minimisation were performed with default restraints on bonding geometry and B-values: 5% of all data were used for Rfree calculation. For the structures 4e2v, 4dg0, 4h7z, 4h6e, 4hqv, 4hsh, 4hqv, 4gcx and “WT”-Tgt·queuine refinement was performed with PHENIX 1.8-1069  with 5% to 10% of all data being used for Rfree calculation and followed by repeated cycles of maximum likehood energy minimization. For the structures 4h7z, 4hvx, 4hqv, 4hsh an additional optimization of the weights between X-ray target and stereochemistry as well as between ADP restraints was performed by PHENIX 1.8-1069 . Amino acid side chains were fitted to σA-weighted 2|Fo| - |Fc| and |Fo| - |Fc| electron density maps using Coot . Ligands were generated using SYBYL 8.0 (Tripos International: 1699 South Hanley Rd., St. Louis, Missouri, 63144, USA). Afterwards, geometric restraints of the ligands were calculated by Monomer Library Sketcher (ccp4) . For structures 4e2v, 4dg0, 4h7z, 4h6e, 4hqv, 4hsh, 4hqv, 4gcx and “WT”-Tgt·queuine water was located using the refinement settings “update waters” implemented in the program PHENIX 1.8-1068 . After further refinement cycles water was checked visually. Glycerol molecules and ligands were located in the difference electron density and added to the model for further refinement cycles. The temperature factors (individual B-factors) for structures 4e2v, 4gcx, 4gd0 and 3bld were anisotropically refined, whereas for structures 4hvx, 4h7z, 4hsh, 4hqv and 4h6e and “WT”-Tgt·queuine TLS refinement was applied. The definition of the TLS groups was done with the TLSMD server . Restraints were applied to bond lengths and angles, planarity of aromatic rings, and Van-der-Waals contacts. Multiple side-chain conformations were built in case an appropriate electron density was observed and maintained during refinement and if the minor populated side chain showed at least 20% occupancy. All final models were validated using PROCHECK . Analysis of temperature factors was done with Moleman .
Alignment and Figures
Alignment of structures based on cα with similar or identical sequences was performed with the alignment function implemented in Pymol (http://www.pymol.org). Figures were prepared using ChemDraw Std 12.0 (PerkinElmer, Massachusetts, USA) and Pymol.
Coordinates of the homology model of the human Tgt catalytic subunit.
Coordinates of the Z.mobilis Tgt(Tyr106Phe) crystal structure determined in in the presence of queuine.
Structure factors of the Z.mobilis Tgt(Tyr106Phe) crystal structure determined in in the presence of queuine.
Overview of crystal structures analysed by Biela et al. (2013).
We gratefully acknowledge the beamline staff at BESSY II (Helmholz-Zentrum Berlin) in Berlin, Germany, for providing us outstanding support. We thank Christian Sohn for his support during “in house” X-ray data collection, François Diederich and Emmanuel Meyer for providing the uncompetitive Tgt inhibitor 2,6-diamino-3H-quinazolin-4-one, Steffi Dörr for exceedingly great technical assistance, Lena Siegling for experimental help during an internship and for editing the manuscript as well as Andreas Blum and Bernhard Stengl for beneficial discussions.
Conceived and designed the experiments: GK KR. Performed the experiments: IB NT FI SG TXPN H-DG AH. Analyzed the data: IB NT AH GK KR. Wrote the paper: KR.
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