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Molecular machines belonging to the AAA+ superfamily of ATPases use NTP hydrolysis to remodel their versatile substrates. The presence of an insertion sequence defines the major phylogenetic pre-sensor I insertion (pre-SIi) AAA+ superclade. In the bacterial σ54-dependent enhancer binding protein phage shock protein F (PspF) the pre-SIi loop adopts different conformations depending on the nucleotide-bound state. Single amino acid substitutions within the dynamic pre-SIi loop of PspF drastically change the ATP hydrolysis parameters, indicating a structural link to the distant hydrolysis site. We used a site-specific protein–DNA proximity assay to measure the contribution of the pre-SIi loop in σ54-dependent transcription and demonstrate that the pre-SIi loop is a major structural feature mediating nucleotide state-dependent differential engagement with Eσ54. We suggest that much, if not all, of the action of the pre-SIi loop is mediated through the L1 loop and relies on a conserved molecular switch, identified in a crystal structure of one pre-SIi variant and in accordance with the high covariance between some pre-SIi residues and distinct residues outside the pre-SIi sequence.
The large AAA+ (ATPases associated with various cellular activities) protein family are responsible for a wide range of ATP-dependent molecular transformations that involve the disassembly and remodelling of protein and nucleic acid complexes (Thomsen and Berger, 2008). Characteristically, all AAA+ members have the ability to self-assemble into higher-order oligomeric structures, usually as hexamers arranged in a ring (Hanson and Whiteheart, 2005). They contain the highly conserved Walker A and Walker B motifs, involved in ATP binding and ATP hydrolysis, the sensor I sequence and the second region of homology that comprises at least one intersubunit catalytic R-finger (Zhang et al., 2002). Sequence insertions prior to the sensor I motif and the preceding α-helix are regarded as a synapomorphic trait that defines the phylogenetic pre-sensor I insertion (pre-SIi) β-hairpin superclade within the AAA+ superfamily (Iyer et al., 2004). AAA+ members belonging to this superclade include HslU, ClpX, Lon, MCM, RuvB, the Ltag helicase and bacterial enhancer binding proteins (bEBPs; Schumacher et al., 2006). Although these sequence insertions (typically 15–25 amino acids in length) are not highly conserved among different AAA+ members, they are generally located in, or at the edge of the inner pore defined by the common hexameric AAA+ ring assembly (Iyer et al., 2004).
In a wide range of bacteria specialized AAA+ proteins (bEBPs), function to activate highly regulated adaptive responses mediated by the enhancer-dependent σ54-containing RNA polymerase (Eσ54) (Studholme and Dixon, 2003; Wigneshweraraj et al., 2008). Upon binding and hydrolysis of ATP, bEBPs remodel the initial closed promoter complexes formed by Eσ54 to create transcriptionally proficient open complexes (Popham et al., 1989). The bEBPs therefore effectively couple ATP hydrolysis to open complex formation where the DNA template strand is loaded within the active site of RNAP (Sasse-Dwight and Gralla, 1988; Morett and Buck, 1989; Popham et al., 1989). The major binding target for bEBPs is the σ54 factor (Bordes et al., 2003). Biochemical and structural analyses of bEBPs PspF, ZraR and NtrC1 (Lee et al., 2003; Rappas et al., 2005; Sallai and Tucker, 2005) have demonstrated that a direct interaction with σ54 occurs via the bEBP-specific GAFTGA motif, located within a structural insertion in Helix 3, termed the L1 loop (Bordes et al., 2003; Chen et al., 2007). The L1 loop is flanked by the pre-SIi [formerly referred to as the L2 loop, Escherichia coli residues 131–139 in PspF (Rappas et al., 2005)], and co-ordinated action between these two loop structures has previously been suggested (Schumacher et al., 2007). Allosteric co-ordination of nucleotide-dependent dynamics between the heterogeneously occupied subunits in the hexameric assembly are important for transcription activation, suggesting that only a subset of subunits directly act on Eσ54 (Joly et al., 2006; Schumacher et al., 2008).
Nucleotide analogues are commonly used to study structural transitions associated with ATP-dependent reactions (Wittinghofer, 1997). The ATP ground state analogue ADP–BeF causes a pronounced rising of the L1 and pre-SIi loops in the bEBP NtrC1, seen using small and wide angle X-ray scattering (SAXS/WAXS) analysis (Chen et al., 2007), a result consistent with the local changes observed in the ATP-bound crystal structure of PspF1−275 (Rappas et al., 2006). Further, σ54 can form stable complexes with NtrC1 and PspF in the presence of ADP–BeF (Chen et al., 2007). Interestingly in SAXS/WAXS analysis, the ATP analogues AMP·PNP and ATPγS did not cause detectable movements in these loop structures, although AMP·PNP was observed to stabilize complexes formed between σ54 and the bEBPs NtrC1 or PspF. Taken together, these results suggest that ATP binding causes the L1 and pre-SIi loops to rise, thereby supporting an initial unstable interaction between the bEBP and σ54 (Chen et al., 2007). Experimentally, stable complex formation between the bEBP and (E)σ54 occurs in the presence of the non-hydrolysable ATP hydrolysis transition state analogue ADP–AlF, which is thought to reflect the conformation of the bEBP–Eσ54 complex near to, or at the point of, an energy coupling step required for reorganization of the Eσ54 closed complex (Chaney et al., 2001; Rappas et al., 2005). ADP–AlF presumably ‘freezes’ the local motions at the ATPase catalytic site, which are linked to other dynamic excursions including the presentation of the L1 and pre-SIi loops to the closed complex.
Here we report a detailed analysis of the function of the flexible pre-SIi loop of PspF1−275. Single amino acid substitutions of the pre-SIi residues (131–139) to alanine invariably impacted on the ATPase kinetics, indicating a strong structural coupling between the ATP hydrolysis site and the distant pre-SIi loop. Differences in the functionalities of the pre-SIi variants enabled three classes of variants to be identified: (i) L1 loop facing; responsible for co-ordinating the position of the L1 loop; (ii) the pre-SIi loop tip; essential for all σ54 interaction and remodelling activities; and (iii) a more variable N-terminal side, which likely serves as a structural scaffold and contains residues important for ATPase activity. Our results establish that specific regions of the pre-SIi loop are important for engaging and remodelling the Eσ54 closed complex in response to different stages of the ATP hydrolysis cycle. We suggest that much, if not all, of the action of the pre-SIi loop is mediated through the L1 loop and relies on a conserved molecular switch, identified in a crystal structure of one pre-SIi variant and in accordance with the high covariance between some pre-SIi residues and distinct residues outside the pre-SIi sequence.
Crystal structures of nucleotide-bound forms of PspF1−275, derived from soaking apo-PspF1−275 crystals with ADP, ATP and AMP·PNP revealed striking and distinct movements of the pre-SIi loop (Rappas et al., 2006). These structures suggest a structural coupling between the nucleotide binding site and the pre-SIi loop (Fig. 1A), which probably reflects nucleotide-dependent movements of the pre-SIi loop in solution. SAXS/WAXS data on the PspF homologue NtrC1 also provide evidence for different conformations of these loops in different nucleotide states (Chen et al., 2007). Figure 1B shows the pre-SIi loop consensus sequence obtained from 289 annotated Pfam (00158) bEBPs sequences. Alignment of these sequences (Fig. 1B) suggests that conservation of the pre-SIi loop (residues 131–139 in PspF) varies, with the RVGG motif (residues 131–134 in PspF, particularly the first glycine present in 99% of the available sequences) being the most conserved segment. To study the function of the pre-SIi loop in PspF, single amino acid substitutions to alanine were made across residues 131–139. For experimental simplicity, we used a structurally characterized form of PspF that is deleted for its DNA binding domain (AAA+ domain residues 1–275; PspF1−275), yet capable of activating transcription from σ54-dependent promoters both in vivo and in vitro from solution (Bordes et al., 2003). Notably, the sequence alignment (Fig. 1B) also indicated that the proline at position 137 in PspF (present in 21% of the available sequences) is replaced by a threonine residue in 14% of bEBPs. In order to ascertain the specific effect of the threonine at position 137, we also constructed a P137T variant.
With the exception of G134A, all clones directed the synthesis of soluble variant forms of PspF1−275. We infer that residue G134, which is located at the tip of the pre-SIi loop (see Fig. 1A), may be required for the structural stability of PspF1−275 because expression was below our detection limit.
The ability of the pre-SIi variants to support transcription activation was assessed using full-length transcription assays on the super-coiled Sinorhizobium meliloti nifH promoter. As shown in Fig. 2A, only two residues (Q136 and P137, lanes 7–9) in the pre-SIi loop were tolerant to alanine (or threonine) substitution, and supported near wild-type (WT, lane 2) levels of full-length transcription. These two residues are located farthest away from the L1 loop (see Fig. 1A) and do not appear to undergo any conformational or rotational changes in the presence of different nucleotides (Rappas et al., 2006). As these residues are not highly conserved among bEBPs (Fig. 1B), we suggest that Q136 and P137 may have little effect on the remodelling activities of PspF1−275 in particular the positioning or stabilization of the σ54 interacting L1 loop. We note that the S135A variant (lane 6) shows significantly reduced activity (compared with lane 2) as do the R131A (lane 3) and L138A (lane 10) variants, but the others are essentially unable to activate transcription.
Using abortive transcription assays (to measure heparin-resistant open complex formation; Wigneshweraraj et al., 2005) with two linear nifH promoter probes, a fully double-stranded (duplex) probe (Fig. 2B) and a pre-opened probe (Fig. 2C; mismatched between positions −10 and −1, thereby mimicking the DNA conformation within the Eσ54 open complex) (Wedel and Kustu, 1995; Cannon et al., 1999), we addressed whether pre-opening the DNA could rescue the transcription activation activity of any of the pre-SIi loop variants. Similar to the full-length transcription assays, only the pre-SIi variants Q136A and P137A/T were able to support open complex formation (Fig. 2B and C, lanes 7–9) at levels comparable to PspF1−275WT (lane 2), even in the presence of pre-opened DNA (Fig. 2C). We also note that the activity of the PspF1−275S135A variant still remained significantly lower than PspF1−275WT (Fig. 2B, lane 6). The remainder of the pre-SIi loop variants demonstrated a significantly reduced ability to support Eσ54 open complex formation. As pre-opening the DNA had little effect on the transcription activation activities of the majority of pre-SIi variants, we suggest that these variants have defects in steps that precede DNA melting. Clearly the pre-SIi loop is important for transcription activation with some residues making greater contributions than others.
To assess the contribution of the pre-SIi loop in supporting σ54 binding and hence the Eσ54 transcription activation activities (of the L1 loop) we used a site-specific protein–DNA cross-linking method to study protein–DNA relationship changes for σ54–DNA, β/β′–DNA and PspF1−275–DNA interactions. The photo-reactive DNA templates were constructed by strategically placing the cross-linking reagent p-azidophenacyl bromide (APAB; Sigma), between positions −1 and +1 (−1/+1) in the context of the duplex, pre-opened and mismatch (at positions −12 and −11, mimicking the DNA conformation of the closed complex) promoter probes. The −1/+1 site was chosen based on previous observations (Burrows et al., 2009) that: (i) only σ54–DNA interactions are detected within the closed complex; (ii) in the ADP–AlF (intermediate) complex σ54–DNA and PspF1−275–DNA cross-linked species are detected; and (iii) only within the open complex are β/β′–DNA interactions observed corresponding to the loading of DNA within the active site of RNAP (Burrows et al., 2008; 2009).
Initially, we analysed a binary σ54–promoter complex formed on the mismatch promoter probe in the presence of PspF1−275 (WT and pre-SIi variants) and dATP. Previously we have shown that PspF1−275WT and dATP can remodel this binary σ54–DNA complex to a ‘supershift’ complex (Fig. 3A labelled σ54ss–DNA; Cannon et al., 2000; 2001). Using this assay, we can establish whether the defects observed in open complex formation by the pre-SIi variants (Fig. 2) are due to an inability to efficiently interact with σ54. In line with the transcription activation data (Fig. 2) only the Q136A, P137A/T and (to a lesser extent) S135A variants supported σ54 supershift complex formation (Fig. 3A, lanes 6–9); however, the remainder of the pre-SIi variants failed to support σ54ss–DNA complex formation (Fig. 3A, lanes 3–5 and 10–11). When these reactions were analysed by cross-linking we observed that where supershift complexes were present, the profile of the cross-linked σ54–DNA species was altered from a single band (Fig. 3A, SDS-PAGE; lane 1 arrowed) to a double band (Fig. 3A, lanes 2 and 7–9, lane 2 arrowed), suggesting that the organization of σ54 is changed in the σ54ss–DNA complex. However, no change in the σ54–DNA profile was observed in reactions containing S135A (Fig. 3A, lane 6), where a weak σ54ss–DNA complex was observed, or the other pre-SIi variants (131–133 and 138–139; lanes 3–6 and 10–11) where no σ54ss–DNA complexes were detected. We also note a weak cross-linked PspF1−275–DNA species was detected in the supershift reactions, particularly with the P137T variant (Fig. 3A, SDS-PAGE; lanes 2 and 7–9, lane 9 arrowed).
In the presence of core RNAP, the Q136A and P137A/T variants (Fig. 3B, lanes 7–9) supported a change in the σ54–DNA interactions (from a single band; lane 1 arrowed, to a double band, lane 7 arrowed) and formation of β/β′–DNA cross-links (lane 9 arrowed) comparable to PspF1−275WT. Together these data confirm that the transcription activation defect associated with some pre-SIi variants is due to their inability to productively interact with σ54 in the σ54–DNA complex or in the Eσ54 closed complex in the presence of dATP. Hence, defects in the pre-SIi variants occur at the level of the σ54 isomerization event, prior to the loading of DNA within the active site of RNAP.
Eσ54 open complex formation requires the coupling of energy derived from bEBP-dependent ATP hydrolysis to remodelling of the Eσ54 closed complex. Effective energy coupling relies on co-ordinated ATP binding and hydrolysis between different subunits of the hexameric PspF1−275 AAA+ ring assembly (Joly et al., 2007; Schumacher et al., 2008). Failure of the pre-SIi variants to activate transcription could therefore be a consequence of a failure to bind or hydrolyse ATP and/or to efficiently couple hydrolysis to restructuring of the Eσ54 closed complex.
To ascertain whether this was the case we measured the ATP binding activities of the pre-SIi variants using non-equilibrium UV cross-linking of [α-32P]-ATP (Schumacher et al., 2004; 2007). Results (Fig. S1) demonstrate that the PspF1−275 pre-SIi variants bind ATP with similar affinity as PspF1−275WT, indicating that the pre-SIi loop does not contribute to the nucleotide binding activities of PspF. In contrast, the pre-SIi variants appear to have a striking effect on the steady-state ATP hydrolysis rates (Table 1). We note however, there is no clear correlation between low ATP hydrolysis rates and defects in transcription activation activity, because the Q136A and T137A variants are similarly active in the transcription assays despite a more than 80% reduction in the ATPase activity of Q136A. The decrease in Vmax observed for all the pre-SIi variants, except P137, indicates a finely tuned coupling between the structure of the pre-SIi loop and the distant ATP active site. These observations functionally distinguish the pre-SIi loop from the adjacent L1 loop, where alanine substitutions do not negatively impact on PspF1−275 ATPase activity (Rappas et al., 2005).
To determine whether the reduced ATP hydrolysis rates observed in the pre-SIi variants are due to defects in hexamer formation, a prerequisite for maximal hydrolysis rates (Schumacher et al., 2004), we performed gel-filtration experiments in the absence and presence of ADP. PspF1−275WT normally exists in equilibrium between a dimer and a hexamer at low protein concentrations (below 10 μM), but in the presence of either ATP or ADP the equilibrium shifts to the hexameric species (Joly et al., 2006). The pre-SIi variants eluted predominantly as dimers (Fig. 4A) in the absence of nucleotide and hexamers in the presence of ADP (Fig. 4B), although we note that the apparent dimer/hexamer ratios differed from PspF1−275WT, especially the V132A, S135A, Q136A and P137T variants. In the case of the S135A and Q136A variants a significant shift towards the hexameric species was observed, whereas the V132A and P137T variants demonstrate a significant defect in their ability to form hexamers, which may account for the reduced ATPase activity of PspF1−275V132A. However, we note that PspF1−275P137T exhibits PspF1−275WT activities in terms of transcription activation and σ54 binding. As none of the pre-SIi variants failed to form the apparent hexameric species in the presence of ADP, we suggest that the lack of ATPase activity for the majority of pre-SIi variants is not simply due to the inability to form a hexamer or bind nucleotide.
To ascertain the contribution the pre-SIi loop makes to PspF1−275 energy coupling activities, nucleotide-dependent interactions between PspF1−275, σ54 and/or Eσ54 promoter complexes were studied using the protein–DNA cross-linking assay and different ATP analogues: (i) the transition state analogue ADP–AlF; (ii) the ground state analogues AMP–AlF and ADP–BeF; and (iii) the slowly hydrolysable ATP analogue ATPγS.
The ability of the PspF1−275 pre-SIi variants to support stable (trapped) complex formation with σ54 and/or Eσ54 was first assayed in the presence of the ATP transition state analogue, ADP–AlF (Fig. 5). As illustrated in Fig. 5A (Native-PAGE), only in the presence of the pre-SIi variants S135A, Q136A and P137A/T were ADP–AlF-dependent trapped complexes formed at a similar level to PspF1−275WT. When these reactions were analysed by photo-cross-linking (Fig. 5A; SDS-PAGE), we observed a σ54-dependent PspF1−275–DNA cross-link (PspF1−275–DNA; Fig. 5A, lanes 6–9 and Burrows et al., 2009). However, we also observed a cross-linked PspF1−275–DNA species in reactions containing the V132A (lane 4 arrowed) and L138A variants (lane 10). These data demonstrate that in the presence of ADP–AlF, the effect of the V132A and L138A substitutions are less apparent than in the transcription assays (Fig. 2), although the stability of ADP–AlF-dependent complexes are greatly reduced (as judged by Native-PAGE analysis; Fig. 5A). Similar to the reactions containing PspF1−275WT, the V132A (lane 4), S135A (lane 6), Q136A (lane 7), P137A/T (lanes 8–9) and L138A (lane 10) variants caused a change in the σ54–DNA profile (Fig. 5A; from a single lane 1 arrowed, to no band lane 6 arrowed). We also observed very weak PspF1−275–DNA interactions with the R131A (lane 3), G133A (lane 5) and Q139A (lane 11) variants, although no alteration in the σ54–DNA profile was evident. Interestingly, when core RNAP was added to these reactions (Fig. 5B) the very weak PspF1−275–DNA interactions with the R131A, G133A and Q139A variants were no longer evident (compare Fig. 5A and B, lanes 3, 5 and 11 respectively); however, we do note a change in the σ54–DNA profile (from a double band to a single band) in the reaction containing the R131A variant (lane 3 arrowed), similar to that observed for PspF1−275WT (lane 2 arrowed) and the V132A, S135A, Q136A, P137A/T and L138A variants (lanes 4 and 6–10).
In the presence of the ATP ground state analogues AMP–AlF (Joly et al., 2008) and ADP–BeF (Burrows et al., 2009), similar to the ADP–AlF reactions, only the S135A, Q136A and P137A/T variants supported stable trapped complex formation (Fig. S2A, Native-PAGE). Importantly, only these variants (S135A, Q136A and P137A/T) supported PspF1−275–DNA interactions (especially in the presence of core RNAP) and an alteration in the σ54–DNA cross-linking profile (from a single band, lane 1 arrowed, to no band, lane 6 arrowed). For the remainder of the pre-SIi variants, no cross-linked PspF1−275–DNA species was detected and neither was a change in the σ54–DNA profile. In the presence of the slowly hydrolysable ATP analogue, ATPγS, we observed a PspF1−275–DNA cross-linked species and an altered σ54–DNA profile with the S135A, Q136A and P137A/T variants (Fig. S3). The S135A variant displays a significantly reduced level of PspF1−275–DNA cross-linked species, which we attribute to the lower ATPase activity of S135A.
Taken together these data indicate that residues V132 and L138 are organized differently with the ATP hydrolysable (dATP and ATPγS) and ATP ground state (AMP–AlF and ADP–BeF) analogues, than with the ATP transition state analogue (ADP–AlF).
Our structural and functional data suggest that (i) pre-SIi residues facing the L1 loop are probably required to position the L1 loop for engagement with σ54 at distinct steps during the ATP hydrolysis cycle and (ii) some pre-SIi residues, despite having no obvious contact features outside the pre-SIi loop, impact on the ATP hydrolysis and σ54 engagement activities of PspF. As the pre-SIi loops of bEBPs demonstrate a degree of sequence conservation (Fig. 1B), this sequence is well suited for predictive covariance analysis as an independent means to identify interacting co-evolved residues. As bEBPs function in a conserved manner, it seems reasonable to suggest that evolutionary variations are susceptible to selective pressures to maintain functionally linked residues. To explore covariation we first aligned the 289 seeded non-redundant sequences of the AAA+ domains of bEBPs (Pfam 00158) using the ClustalW program. Using three established covariance algorithms (Fodor and Aldrich, 2004) [observed minus expected squares, statistical coupling analysis and McLachlan-based substitution correlation (Olmea et al., 1999)] we determined the covariance of residues within the conserved pre-SIi sequence and the entire AAA+ domain of bEBPs (Fig. S4). We also determined the covariance between PspF residues 80–98 (which includes the L1 loop sequence) and the PspF pre-SIi loop sequence (Fig. 6A). As shown in Fig. 6A PspF residue E97 (arrowed) exhibits strong covariance with pre-SIi residue R131 and residue E81 (arrowed) exhibits covariance with the pre-SIi residues R131, G134 and L138, supporting the existence of a functionally conserved mechanism by which bEBPs relate the nucleotide-bound state to pre-SIi loop dynamics.
The severely reduced ATP hydrolysis rates observed for the majority of the pre-SIi variants suggest the existence of an important structural link coupling the pre-SIi loop to the distant ATP hydrolysis site. We reasoned that mutations in the pre-SIi loop would result in local, and potentially global, conformational changes that could reveal mechanistic details of this structural link. Based on our covariance analysis we determined the crystal structure of apo-PspF1−275R131A in order to determine the effect of the R131A mutation on the conformation of the pre-SIi loop compared with apo-PspF1−275WT (Fig. 6B and Fig. S5A–C). Clear local differences are evident in the conformation of the pre-SIi loop, as well as a significant rotation in the side-chain of residue E81 of the adjacent L1 loop (Fig. 6B). These observations strongly support the view that residue R131 of the pre-SIi loop communicates with residue E81 of the L1 loop in a nucleotide-dependent manner that appears essential for PspF1−275 activity. Disruption of the R131-E81 link (by introduction of the R131A mutation) causes the pre-SIi to rotate, so that the alanine side-chain is now pointing towards the other stem of the pre-SIi loop (away from the L1 loop). More globally, the alanine substitution at residue R131 results in conformational changes in Helix 4 (most notably residue E125) and, somewhat surprisingly, the orientation of residue R168 a putative R finger (as shown by the root mean square deviation plot between PspF1−275R131A and PspF1−275WT; Fig. S5D). Although these differences are modest, they are the most pronounced changes evident over the entire length of the PspF1−275 structure outside the pre-SIi and L1 loops.
We have systematically examined the activities of the pre-SIi sequence in PspF1−275, characterized by crystallographic studies as a well-defined loop structure that changes its organization and orientation in the presence of different nucleotides (Rappas et al., 2006). In PspF1−275 and the related bEBPs NtrC1 and ZraR, a direct interaction between the pre-SIi loop and the L1 loop is evident (Lee et al., 2003; Sallai and Tucker, 2005). The importance of specific pre-SIi residues in PspF1−275 functionality now establishes that particular regions of the pre-SIi loop are important for engaging and remodelling the Eσ54 closed complex in response to the ATP hydrolysis cycle.
The majority of the pre-SIi variants showed no marked defects in self-association, although we do note that the V132A and P137T variants exhibited lower levels of hexamer formation (which may account for the low ATPase activity of V132A) and the S135A and Q136A variants showed a propensity for the hexameric state (even though the ATPase activity of S135A is severely reduced). Taken together these results suggest that the pre-SIi loop does not contribute greatly to the energetically favourable interactions (at the protomer–protomer interface) needed for hexamer formation. Clearly, alanine substitutions in the pre-SIi loop impact on the catalytic site architecture, reflected by the decrease in ATP hydrolysis rates. Differences in KM, notably for the V132A and S135A variants probably reflect differences in hydrolysis rates rather than in ATP binding due to the reported high off-rates (Rombel et al., 1999; Schumacher et al., 2004). The similar apparent nucleotide binding affinities of all the pre-SIi variants tested (Fig. S1) are consistent with the spatial separation of residues involved in nucleotide binding and hydrolysis (Rappas et al., 2005). Apart from the P137A/T variants, all the pre-SIi variants showed drastically reduced ATP hydrolysis rates, which is notable because the pre-SIi is a flexible surface-exposed loop that is spatially distant from the ATP hydrolysis site, suggesting that linked dynamic modes underpin the nucleotide-dependent functions of PspF (Rappas et al., 2006).
The crystal structure of apo-PspF1−275R131A illustrates that destabilization of the pre-SIi loop–L1 loop interaction results in a significant conformational change in the pre-SIi loop that propagates to the C-terminal moiety of Helix 4 (Fig. 6B). This change appears to weaken the intrasubunit E125–R168 interaction and the orientation of the putative R-finger residue R168. Previously we showed that the R168A variant forms nucleotide-independent hexamers that are ATPase defective (Schumacher et al., 2004). These prior observations suggested that residue R168 inhibits hexamer formation in apo-PspF1−275WT while being required for intersubunit catalysis in the ATP-bound state (Schumacher et al., 2004). Consistent with these findings, we propose that the structural conformation of the pre-SIi loop of apo-PspF1−275WT, via Helix 4 residue E125, supports a conformation of R168 that inhibits self-association.
Using different ATP analogues three broad classes of activities associated with the pre-SIi loop were identified. Class I contained variant forms of the pre-SIi loop that had activities that were indistinguishable from PspF1−275WT, indicating that these pre-SIi residues (Q136 and P137) are largely unimportant for nucleotide-dependent engagement of the Eσ54 closed complex. We also assign S135 to class I because it behaves similarly to PspF1−275WT in the nucleotide-dependent interaction studies and the significantly reduced transcription activation and σ54 isomerization activities could be attributable to its low ATPase activity. These residues are located farthest away from the L1 loop (Fig. 1A) and are therefore unlikely to interact with the L1 loop. Class II variants (G133, Q139 and to some extent R131) essentially failed in all the nucleotide-dependent interaction assays tested. The severe functional defects observed for PspF1−275G133A are not surprising given its high sequence conservation and high –ψ angle indicating that backbone flexibility at the tip of the pre-SIi loop appears indispensable for bEBP activity. Crystal structures of PspF1−275 illustrate that nucleotide binding causes the pre-SIi loop to twist around its longitudinal axis (Rappas et al., 2006). Diminishing the glycine-associated flexibility (in the G133A variant) strongly suggests that the potential for ‘structural twist’ is critically important for PspF functionality. Class II variants maintain the nucleotide binding and self-association activities but cannot engage the Eσ54 closed complex, presumably because the contact features for binding σ54 (i.e. the L1 loop) are inappropriately presented. Class III variants (represented by V132A and L138A) supported PspF1−275–DNA cross-links in the presence of the ATP transition state analogue (ADP–AlF) but not with the ATP ground state analogues (AMP–AlF and ADP–BeF) or the slowly hydrolysable ATP analogue (ATPγS), suggesting that the pre-SIi loop plays at least two distinct roles in productive Eσ54–PspF interactions that are dependent on the nucleotide state: weak interactions that exist in the nucleotide ground state and strong interactions in the ATP transition state.
The high probability of pair-wise co-evolution of the L1 residues E81 and E97 (in PspF) with the pre-SIi residue R131 (in PspF) suggests that functionally important contacts between the pre-SIi and L1 loops exist which may provide a mechanistic rational for how different nucleotide states could orientate the L1 loop for Eσ54 engagement. R131 would function as switch which pivots between E81 in the ATP ground state and E97 in the ATP transition state. Disruption of this switch may account for the failure of PspF1−275R131A to stably interact with σ54, as demonstrated by the lack of σ54-dependent PspF1−275–DNA cross-links with the R131A variant in the presence of the metal fluoride analogues (Fig. 5 and Figs S2 and 3, lane 3). The covariance of residues E81 (L1 loop) and R131, G134 and Q136 (pre-SIi) indicates that additional residues are required for maintaining a pre-SIi loop conformation suitable for a productive E81–R131 interaction to occur (Fig. 6A). Overall, the functionally important R131-E81/E97 switch (studied in PspF) appears highly conserved within the bEBP family.
The DNA-bound model of the electron microscopy structure of Eσ54-PspF1−275:ADP–AlF indicates that the pre-SIi loop lies proximal to both σ54 and promoter DNA (Bose et al., 2008). One important observation from the nucleotide-dependent studies is that in the presence of different DNA templates (Fig. 5 and Figs S2 and 3) no large scale changes in the amounts of complexes formed (in Native-PAGE analysis compared with PspF1−275WT) were observed, nor was the stability of these complexes increased or reversed, inferring that the pre-SIi loop does not directly contact promoter DNA and/or σ54. In contrast, interactions between σ54 and the L1 loop variant PspF1−275T86S can be recovered when promoter DNA sequences downstream of the −12 position are missing (Dago et al., 2007). We propose that much of the action of the pre-SIi loop is manifest through the L1 loop interacting with σ54 and that the pre-SIi loop in PspF and other related bEBPs works mainly on the L1 loop rather than its substrate.
The similarity in the location of the synapomorphic pre-SIi feature, which is found in or at the edge of the inner pore of the hexameric AAA+ ring assembly (Iyer et al., 2004), raises an important question regarding a common role for the pre-SIi in other AAA+ proteins. In RuvB, which contacts RuvA via the pre-SIi β-hairpin, mutations in the pre-SIi result in decreased RuvB ATPase activity (Han et al., 2001; Yamada et al., 2002), while in E1 helicase of Papilloma virus, the pre-SIi β-hairpin interacts with single-stranded DNA (Enemark and Joshua-Tor, 2006). In these cases the pre-SIi contacts auxiliary proteins or substrates directly, for which we found no evidence in PspF. In MCM, a pre-SIi mutation modestly increased the Kd for DNA binding, but significantly reduced ATPase and abolished helicase activity (McGeoch et al., 2005), suggesting tight structural coupling between the pre-SIi and the hydrolysis site, similar to our observations with PspF. Distinct functional roles that depend on the nucleotide-bound state have, as far as we know, not been shown for other AAA+ pre-SIi sequences. However, structural studies of the E1 helicase (Enemark and Joshua-Tor, 2006) and the E1-related Ltag helicase (Gai et al., 2004) suggest that different nucleotide states result in distinct orientations of the pre-SIi. More recently, nucleotide state-dependent dynamics for the pre-SIi have also been proposed for MCM (Barry et al., 2009) and ClpX (Martin et al., 2008a,b;).
Clearly, the divergence in pre-SIi sequences among members of the pre-SIi β-hairpin superclade of AAA+ proteins and their distinct direct or indirect involvements in substrate remodelling do not allow the simple assignment of common roles to this structural feature. Rather, the strategic placement of the pre-SIi near or in the pore of the AAA+ ring assembly, and the potential structural coupling to the ATP hydrolysis event may explain the marked evolutionary prevalence of the pre-SIi.
Escherichia coli core RNAP was purchased from Epicentre technology (Cambio). Klebsiella pneumoniaeσ54 was purified as described (Wigneshweraraj et al., 2003). Plasmid pPB1 encoding Escherichia coli PspF residues 1–275 (PspF1−275 with an N-terminal His6 tag in pET28b+) was mutagenized (Quickchange Mutagenesis Kit, Stratagene) resulting in plasmids pPB1(R131A), pPB1(V132A), pPB1(G133A), pPB1(G134A), pPB1(S135A), pPB1(Q136A), pPB1(P137A), pPB1(P137T), pPB1(L138A) and pPB1(Q139A). Proteins were overproduced as described (Wigneshweraraj et al., 2003). Proteins were purified using a gravity flow method. Briefly Ni-NTA resin (Qiagen) was equilibrated with buffer ANI (20 mM sodium phosphate pH 7.0, 500 mM NaCl, 5% (v/v) glycerol) prior to applying the cell supernatant. The resin was then washed with buffer ANI, followed by wash buffer 1 (buffer ANI plus 40 mM imidazole) and wash buffer 2 (buffer ANI plus 80 mM imidazole). The protein was eluted using buffer BNI (buffer ANI plus 1 M imidazole). The S. meliloti nifH phosphorothioated (Operon) DNA probes were derivatized with p-azidophenacyl bromide as described (Burrows et al., 2004). The modified promoter strands were 32P labelled and annealed to the complementary strand as described (Wigneshweraraj et al., 2003; Burrows et al., 2008).
Full-length or abortive transcription assays were performed in STA buffer (25 mM Tris-acetate pH 8.0, 8 mM Mg-acetate, 10 mM KCl, 3.5% w/v PEG 6000) in a 10 μl reaction containing 100 nM Eσ54 (reconstituted at a 1:4 ratio of E:σ54), 4 mM dATP and 20 nM promoter DNA probe. The mix was incubated at 37°C for 5 min and the reaction started by addition of 5 μM PspF1−275WT or variants and incubated for a further 10 min at 37°C. Full-length transcription was initiated by adding an elongation mix containing 100 μg ml−1 heparin, 1 mM ATP, CTP, GTP, 0.05 mM UTP and 3 μCi [α-32P]-UTP and incubated at 37°C for 20 min. The full-length transcription products were analysed on a 6% denaturing gel. Synthesis of the abortive transcript (5′ UpGGG) was initiated by adding an abortive mix containing 100 μg ml−1 heparin, 0.5 mM 5′ UpG and 4 μCi [α-32P]-GTP and incubated at 37°C for 20 min. The abortive transcription products were analysed on a 20% denaturing gel. Full-length and abortive transcription gels were visualized and quantified using a Fuji FLA-5000 PhosphorImager.
ATP binding assays of PspF1−275 proteins by UV cross-linking were performed as described (Schumacher et al., 2004). ATPase reactions were carried out as described (Schumacher et al., 2008). ATPase assays were performed in reaction buffer (35 mM Tris-acetate pH 8.0, 70 mM K-acetate, 5 mM Mg-acetate, 19 mM ammonium acetate, 0.7 mM DTT) containing 15 mM MgCl2 and incubated at 23°C, using 0.06 μCi [α-32P]ATP or [α-32P]-dATP as nucleotide tracers. Prior to ATP titration experiments, protein concentration titrations were carried out at 0.1 mM ATP to verify maximal turnover rates were achieved. Reactions were quenched with 5 vols of 2 M formic acid. [α-32P]-ADP was separated from [α-32P]-ATP by thin-layer chromatography [on Polygram Cel 300 PE (polyethyleneimine)] and visualized and quantified using a Fuji FLA-5000 PhosphorImager. ATP titration experiments and all PspF1−275 titrations were designed so that only 10–30% of the initial amount of ATP was hydrolysed thereby ensuring that any ADP produced had no measurable effect on ATP hydrolysis rates. It also ensures that ATP was not limiting in the assays and that non-linearity of turnover rates was minimal. Vmax and Km values as well as standard errors were determined at initial concentrations of 0.05–1 mM ATP using non-linear regression Graphit software (Erithacus Software Limited).
Gel filtration chromatography was carried out with 50 μM PspF1−275 (WT and variants) at room temperature in running buffer (20 mM Tris pH 8.0, 50 mM NaCl, 15 mM MgCl2, 0.02% (w/v) azide) at a 0.7 ml min−1 flow rate using a BioCad Sprint HPLC system and a Bio-Sep-S 3000 column (Phenomenex). To test for nucleotide-dependent oligomerization the column was pre-equilibrated with five bed volumes of 0.5 mM ADP, prior to loading 10 μM PspF1−275 (WT or variants), supplemented with 0.5 mM ADP. The column was calibrated using molecular weight standards (Sigma): Blue Dextran (200 kDa), Thyroglobulin (669 kDa), Ferritin (440 kDa), Catalase (232 kDa), Aldolase (158 kDa), Albumin (67 kDa), Ovalbumin (43 kDa), Chymotrypsin (25 kDa) and Ribonuclease (13.5 kDa).
Cross-linking reactions were conducted at 37°C in STA buffer in a 10 μl reaction volume as described (Burrows et al., 2008; 2009). Briefly, where indicated either 1 μM σ54 or 200 nM Eσ54 (reconstituted using a 1:2 ratio of E:σ54) and 20 nM modified 32P-labelled promoter DNA probe was incubated for 5 min at 37°C. Open complexes were formed by 4 mM dATP and 5 μM PspF1−275 and the reaction incubated for 10 min at 37°C. Trapped complexes were formed in situ by adding 5 μM PspF1−275, 5 mM NaF and either 1 mM ADP, 0.2 mM BeCl3 for the ADP–BeF reactions; 1 mM ADP, 0.2 mM AlCl3 for the ADP–AlF reactions; and 1 mM AMP, 0.2 mM AlCl3 for the AMP–AlF reactions and incubated for 10 min at 37°C. To eliminate free core RNAP from binding the promoter probe, reactions contained 100 ng ml−1 salmon sperm DNA. Reactions were UV irradiated at 365 nm for 30 s using a UV-Stratalinker 1800 (Stratagene). A 2 μl sample of the reaction was analysed by Native-PAGE (4.5%), run at 100 V for 55 min. The remainder of the cross-linking reaction was diluted using 5 μl 10 M Urea and 5 μl 2× SDS loading buffer (Sigma), heated at 95°C for 3 min and 10 μl loaded on a 7.5% SDS-PAGE gel run at 200 V for 50 min. The gels were visualized and quantified using a FLA-500 PhosphorImager. The cross-linked proteins were identified using antibodies as described (Burrows et al., 2008).
Covariance analysis was performed as described (Fodor and Aldrich, 2004). Briefly, the 289 sequences in Pfam (00158) were first aligned using ClustalW. For a multiple alignment of N sequences, an NxN matrix (with dimensions k and l) was constructed for each pair of residues (i and j). Each entry in the matrix was then scored using the McLachlan substitution matrix (Olmea et al., 1999), producing high scores for identities/conservative substitutions and low scores for non-conservative substitutions. The correlation between the two columns (i and j) was calculated using the equation where <S> is the average and σi is the standard deviation of all entries in the matrix.
PspF1−275R131A was expressed, purified, crystallized and flash frozen as described (Rappas et al., 2005). Diffraction data were collected (in-house) using a March 345 image plate mounted on a Rigaku RU-H3RHB rotating-anode X-ray generator (operated at 50 kV and 100 mA) fitted with Osmic confocal optics and a copper target (Cu Kα; λ= 1.542 Å). All the data sets were processed using MOSFLM (Leslie, 1992) and SCALA (Evans, 2006) using the CCP4 program suite (Collaborative Computational Project, 1994). Phases for PspF1−275R131A crystals were obtained by molecular replacement using the PspF1−275WT (PDB 2BJW) structure as a search model and the PHASER program (Storoni et al., 2004). Flexible regions such as the L1 (residues 79–93) and pre-SIi loops were first removed from the search model and built-in during rounds of refinement. The Fo-Fc and 2Fo-Fc maps showed some connected electron density for residues 79–81, 91–93 and 129–135, which were manually built-in using program O (Jones et al., 1991). After several rounds of rebuilding, minimization and B-individual refinements, water molecules were added in the Fo-Fc map automatically (using CNS) and manually. A final cycle of TLS refinement was carried out using the REFMAC5 program (Murshudov, 1997) and the two TLS groups: the α/β subdomain (residues 7–177) and the α-helical domain (residues 180–255). The refinement statistics are summarized in Table S1. All figures were prepared using Pymol (DeLano, W.L. The PyMOL Molecular Graphics System 2002).
This work was supported by project grants to M.B. from the Wellcome Trust and BBSRC and by a grant to B.T.N. from the NIH (GM069937). We thank Dr N. Joly for his help with the AMP–AlF trapping reactions and Mr C. Engl and Miss E. James for valuable comments on the manuscript. We also thank Sarah Butcher from the bioinformatics service for her advice and the members of Professor Buck's laboratory for helpful discussions and friendly support.
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