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Mtr4p is a DEVH-box helicase required for 3′-end processing and degradation of various nuclear RNA substrates. In particular, Mtr4p is essential for the creation of 5.8S rRNA, U4 snRNA, and some snoRNAs, and for the degradation of cryptic unstable transcripts (CUTs), aberrant mRNAs and aberrant tRNAs. Many instances of 3′-end processing require limited polyadenylation to proceed. While polyadenylation can signal degradation in species from bacteria to humans, the mechanism whereby polyadenylated substrates are delivered to the degradation machinery is unknown. Our previous work has shown that Mtr4p preferentially binds poly(A) RNA. We suspect that this preference aids in targeting polyadenylated RNAs to the exosome. In these studies, we have investigated the mechanism underlying the preference of Mtr4p for poly(A) substrates as a means to understand how Mtr4p might facilitate targeting. Our analysis has revealed that recognition of poly(A) substrates involves sequence-specific changes in the architecture of Mtr4p-RNA complexes. Furthermore, these differences significantly affect downstream activities. In particular, homopolymeric stretches like poly(A) ineffectively stimulate the ATPase activity of Mtr4p and suppress the rate of Mtr4p-RNA complex dissociation. These findings indicate that the Mtr4p-poly(A) complex is unique and ideally suited for targeting key substrates to the exosome.
Quality control of nuclear RNA requires both processing and surveillance pathways. In particular, ribosomal (rRNA), small nucleolar (snoRNA), small nuclear (snRNA) and messenger (mRNA) RNAs are all transcribed as precursor RNAs (pre-RNAs) which must then be cleaved and/or trimmed to produce functional RNAs (1). Any byproducts from the conversion of pre-RNA to functional RNA must be rapidly degraded. Likewise, many aberrant RNAs are subjected to surveillance and thereby eliminated from the nuclear RNA pool to maintain proper cell function. The nuclear exosome is the major degradation machine involved in both pathways of nuclear RNA quality control. In Saccharomyces cerevisiae (S. cerevisiae), the nuclear exosome is a collection of six RNase PH homologues (Rrp41p, Rrp42p, Rrp43p, Rrp45p, Rrp46p and Mtr3p) which are inactive and form a scaffolding ring structure (2), three putative RNA binding proteins (Rrp4p, Rrp40p and Csl4p) which form a cap on the RNase PH hexamer (3), and two active 3′→ 5′ exonucleases Rrp44p (2-4) and Rrp6p (5, 6). Rrp44p also possesses an endonuclease domain that is important for exosome function. Many exosome substrates contain structured segments that preclude complete processing or degradation by the exosome alone, thus requiring cofactors to ensure the generation of the desired end product. One of those cofactors, Mtr4p, is an indispensible partner of the exosome, and is likely responsible for maintaining the momentum of exonucleolytic activity as both Mtr4p and the exosome move through structured regions of some RNA substrates. Mtr4p has been linked to the processing of a diverse population of pre-RNAs. In conjunction with the exosome, Mtr4p assists in processing the 7S rRNA precursor to produce 5.8S rRNA, an essential component of the 60S ribosomal subunit (7). Mtr4p is also required for processing some snRNAs and snoRNAs (8). Specifically, Mtr4p is involved in the 3′ end maturation of U4 snRNA, a part of the U4/U5·U6 trimer which is recruited during spliceosome assembly (7). In addition to its processing function, Mtr4p participates in the nuclear surveillance pathway that degrades aberrant RNAs. Mtr4p helps degrade aberrant mRNAs such as those modified by inappropriate adenylation, splicing, or other abnormalities (9, 10). Some of the surveillance activities of Mtr4p are performed in the context of the TRAMP (Trf-Air-Mtr4 polyadenylation) complex. TRAMP is a three-protein complex consisting of Mtr4p, a poly(A) polymerase (Trf4p or Trf5p), and a zinc-knuckle protein (Air1p or Air2p) (11, 12). As part of the TRAMP complex, Mtr4p participates in both rRNA and snoRNA surveillance (9, 13, 14). Mtr4p also assists in TRAMP-assisted degradation of hypomodified tRNAiMet (12, 15, 16) and cryptic unstable transcript RNAs (CUTs) (12, 15-18).
Mtr4p belongs to the Ski2-like family of DExH and DExD-box helicases within Superfamily 2 and possesses both RNA-dependent ATPase activity and ATP-dependent 3′→ 5′ RNA helicase activity (16, 19). Genetics experiments have shown that depletion of Mtr4p in cells is lethal and that the helicase motifs of Mtr4p are critical for its function in vivo. In particular, mutations of the conserved lysine in motif I (Lys-177) or of the conserved serine of motif III (Ser-293) result in dominant negative growth defects (20). Recent crystal structures of apo Mtr4p (21) and an Mtr4p-ADP-RNA (22) complex reveal that the canonical recA-like core domains are decorated with both winged-helix and seven-helix bundle domains similar to those found in the related archaeal Hel308 helicase (23) and a novel arch domain. The arch domain is both unique to the Ski2-like helicases and essential for Mtr4p function (21). Such unique sequence and structural features of Mtr4p and related helicases likely contribute to attributes which differentiate them from other enzymes in the same superfamily. One remarkable feature of Mtr4p is its distinct preference for binding short poly(A) tracts (19). While previous studies identified this preference, the factors that control selective binding to poly(A) substrates are not well-understood. Further, the parameters that define a stable Mtr4p-RNA complex as a function of RNA sequence have yet to be determined. Finally, the extent to which sequence-specific interactions affect downstream activities such as ATPase activity is unclear. Thus, we undertook a series of experiments to quantitatively assess the impact of RNA substrate sequence on the affinity and stability of Mtr4p-RNA complexes and the efficiency with which Mtr4p hydrolyzes ATP.
The ability of Mtr4p to recognize free 3′-poly(A) tails generated by TRAMP-mediated polyadenylation is a prerequisite for exosome-mediated cleavage of those substrates, as depletion of Mtr4p in vivo gives rise to extended polyadenylated forms of a variety of nuclear RNAs (7, 8, 24). Thus, understanding the mechanism whereby Mtr4p recognizes poly(A) RNA is key to understanding how Mtr4p promotes processing of TRAMP substrates by the exosome. It is possible that such recognition leads directly to Mtr4p-mediated recruitment of the exosome for processing. The ability of Mtr4p to both remodel structured RNA and target polyadenylated substrates to the exosome would be advantageous for promoting the processing and degradation of highly-structured substrates.
In this study we report that both substrate sequence and nucleotide-bound state have a striking effect on the biochemical properties of Mtr4p-RNA complexes. In particular, we show Mtr4p binds poly(A) via a novel mechanism that generates a different architecture for the Mtr4p-poly(A) complex than for other complexes. We also show that poly(A) suppresses both ATPase activity and complex dissociation relative to the random-sequenced substrate. Taken together, our data show that the Mtr4p-poly(A) interaction is uniquely configured to promote targeting. Further, some unique properties of the Mtr4p-poly(A) interaction exist independent of ATPase activity, indicating that one role of Mtr4p is to discriminate between substrates and thereby maintain contact with the short polyadenylated sequences which signal degradation.
Recombinant S. cerevisiae Mtr4p was expressed and purified as previously described (19). We evaluated the homogeneity of the protein in solution (typical particle size ~ 12 nm) using dynamic light scattering in a Zetasizer Nano S (Malvern Instruments). Recombinant Mtr4p was snap frozen and stored at −80 °C.
Synthesis, 2′ hydroxyl deprotection, and purification of the RNA substrates (shown in Table 1) used in this study were performed by Dharmacon Research or Integrated DNA Technologies. Fluorescein groups were linked to the 5′-ends of some of the RNA substrates during solid-phase synthesis and are designated by the prefix “Fl” where applicable. Lyophilized RNA samples were resuspended in 1X TE buffer. RNA yields were quantified by absorbance spectroscopy at OD 260nM in a Beckman DU-640 spectrophotometer and the ε260 of each of the substrates, provided by the manufacturer. Fluorophore labeling efficiencies were quantified by absorbance, incorporating fractional contributions of coupled fluorophores to OD260 for substrates containing fluorescein (Fl) moieties as previously described (25).
These four different 20 nucleotide RNA sequences were chosen for their similarity to potential in vivo substrates and their limited propensity to form higher order structures. The substrate length (20 nt) reflects the average number of adenylates added by the Trf4p polymerase of the TRAMP complex to hypomethylated pre-tRNAiMet in vivo (15). One substrate is a purine homopolymer (A20). The addition of a poly(A) tail is a known degradation signal for RNAs within the nucleus (11, 12). Poly(A) substrates can form a single helix in solution (26), but when interacting with poly(A)-binding proteins generally show an extended poly(A) structure (27, 28). The second substrate contains a random sequence (R20) and was designed to represent general RNA. Specifically, the R20 substrate was designed to lack both repetitive sequences and significant secondary structure (as determined by RNA structure prediction programs (29, 30)). The third substrate, a pyrimidine homopolymer (U20) was used to control for effects that are due to the presence of a homopolymer and are not specific to poly(A). At low temperatures poly(U) substrates can fold to form hairpins that result in double-helical structures (31). To evaluate potential consequences of the U20 substrate forming higher order structures as a factor in our results, we inserted alternating cytosines in the U20 substrate which are expected to eliminate any propensity to form such structures, thereby creating the fourth substrate ((UC)10).
The average size of the Mtr4p binding site to the RNA substrates A20 and R20 (Table 2) was determined as a function of nucleotide-bound state using the model-independent Macromolecular Competition Titration Method (MCT) of Jezewska and Bujalowski (32, 33). This quantitative approach determines the free protein concentration (PF) and binding density (Σν) for isotherms describing association of a ligand (i.e., Mtr4p, in this study) to a macromolecule (i.e., fluorescein-labeled RNA, or Fl-RNA). We define binding density as the average number of Mtr4p proteins bound per strand of Fl-RNA. These thermodynamic parameters were extracted from analysis of a series of Mtr4p protein titrations against at least three different RNA concentrations. The total RNA population consisted of 1 nM Fl-RNA supplemented with increasing amounts of equivalent-sequence but nonfluorescent RNA competitor (typically 5 to 45 nM final RNA concentration) to generate binding isotherms that were shifted to higher protein concentrations. The anisotropy measurements were conducted using a Beacon 2000 Variable Temperature Fluorescence Polarization System equipped with fluorescein excitation (485 nm) and emission (535 nm) filters. A typical reaction (100 μl) contained a limiting concentration (1 nM) of an Fl-RNA substrate, binding buffer (10 mM Tris-HCl pH 8, 40 mM NaCl, 2 mM dithiothreitol, 1 mM Adenosine 5′-(β,γ-imido)triphosphate (AMP-PNP) or ADP, and 5 mM MgCl2 when indicated), and an increasing concentration of protein (0 - 2.5 μM). In addition, a second set of reaction conditions was used to aid in determining the effects of salt concentrations closer to the physiological range on the reaction. The buffer system for those experiments contained 5 mM Tris-HCl pH 8, 2 mM dithiothreitol, 90 mM potassium acetate, and 1 mM magnesium acetate (34-37). The polarimeter was operated in static mode using a single sample containing all components, except the labeled RNA and protein, which was read as a blank before the experiment began. Samples were incubated following addition of the labeled RNA until they reached equilibrium before anisotropy was measured. The equilibration time was determined by the dissociation kinetics measurements, to be either 1 min for R20, or 30 min for A20. Mtr4p-RNA binding was monitored by the net change in fluorescence anisotropy, ΔAobs = Ax − A0, where Ax is the observed anisotropy in the presence of x nM Mtr4p and A0 is the anisotropy in the absence of protein. Because ΔAobs is exclusively determined from the extent of ligand (Mtr4p) binding to the Fl-RNA, all curves span the same anisotropy range and plateau to the same maximum value at saturation. The isotherms shift to the right in the presence of increased non-fluorescent RNA competitor concentration (RC) because more protein is necessary to saturate the competing lattice. ΔAobs reflects the population-weighted average of contributions from all Mtr4p-Fl-RNA complexes, each with its own intrinsic anisotropy contribution ΔAj for the j-th species. Since ΔAobs is correlated to a unique distribution of Mtr4p-Fl-RNA complexes, a pair of RNA competitor and total protein concentrations (RC1, PT1) obtained from one isotherm at a given ΔAobs has the same PF and ΣνR as the concentration pair (RC2, PT2) which possesses the same ΔAobs in a second isotherm. ΣνR denotes the binding density of Mtr4p to Fl-RNA, where “R” indicates “reference.” By conservation of mass, for any two total protein concentrations PT1 and PT2 which have equal ΔAobs values when titrating against unlabeled RNA concentrations RC1 and RC2 in the presence of a common concentration of labeled RNA (e.g., RR = 1 nM),
and the free protein concentration is calculated by:
where i = 1 or 2, denoting the specified protein concentrations PT1 versus PT2 or RC1 versus RC2. This analysis requires no prior knowledge of the binding mechanism, and makes no assumptions about the relative Mtr4p binding affinity to Fl-RNA or competitor RNA (i.e., the analysis is applicable regardless of whether ΣνR and ΣνC are the same or different). In any case, plotting the anisotropy change, ΔAobs, as a function of ΣνC allows one to obtain the binding stoichiometry of the Mtr4p-nonfluorescent RNA complex (Figure 1). The correlation of ΣνR to ΔAobs and to PF in the absence of competitor can be determined by Macromolecular Binding Density Analysis (MBDA) (33, 38) of analogous protein titrations against a series of Fl-RNA concentrations (with no unlabeled competitor). Given ΣνC derived from MCT analysis and using the ΔAobs to calculate ΣνR using the relationship obtained from MBDA, the unbound protein concentration PF is obtained from Equation 4 and can be independently validated by comparison to the PF found from MBDA. In this way, the free protein concentration, as well as the population-averaged binding densities of unlabeled RNA (ΣνC) and Fl-RNA (ΣνR), is calculable without approximation or any assumptions about the binding mechanism.
RNA binding affinity was measured using a fluorescence anisotropy based assay according to the method of Brewer and colleagues (25, 39). The anisotropy measurements were conducted under the same solution conditions as described for MBDA above. A typical reaction (100 μl) contained a limiting concentration (0.2 nM) of an RNA substrate labeled with fluorescein at its 5′-end, binding buffer (with 1 mM AMP-PNP or ADP, and 5 mM MgCl2, when indicated), and an increasing concentration of protein (0 - 2.5 μM). The equilibration time was determined by the dissociation kinetics measurements to be either 30 min for A20, and A10 substrates or 1 min (all other substrates). The total intensity of emission was monitored concurrent with anisotropy to ensure that interactions between Mtr4p and the RNA substrate did not affect the quantum yield of the fluorophore. In cases where the total fluorescence emission varied as a function of added protein concentration, an appropriate correction factor (40-42) was applied to the measured anisotropies. Single-site equilibrium association constants were calculated from the binding data using GraphPad Prism version 3.03 and Equation 5 (25):
where Atotal represents the total anisotropy, ARNA is the intrinsic anisotropy of the RNA in the absence of protein, Acomplex is the anisotropy of the saturated protein-RNA complex, [P] is the protein concentration, and Ka is the association constant. This binding model assumes that one binding site (or multiple equivalent binding sites) exists on the substrate RNA. The appropriateness of the single binding site model was evaluated by the agreement between the observed and calculated binding isotherms and the random distribution of residuals. In cases where the single-site model was deemed inappropriate, binding isotherms were analyzed using a variant of the Hill equation (43):
where Atotal is the measured anisotropy, Acomp is the anisotropy of the saturated protein-RNA complex, ARNA is the inherent anisotropy of the RNA substrate, and h is the Hill coefficient. This equation returns an estimate of the amount of protein required to achieve half-maximal signal intensity ([P]1/2) which, in the case of a single binding site (i.e. h = 1.0), is equivalent to the Kd.
A coupled pyruvate kinase-lactate dehydrogenase assay was used to assess the Michaelis-Menten kinetics of ATPase activity as described (44) with minor modifications. Briefly, Mtr4p (100 nM) was incubated with varying concentrations of ATP (0 – 5 mM) and either 250 nM RNA or 500 nM RNA, depending on the Km of the particular RNA, at 37 °C. A typical reaction of 0.5 ml contained; 50 mM Sodium HEPES, pH 7.5, 50 mM NaCl, 5 mM MgCl2, 0.1 mM EDTA, 1 mM dithiothreitol, 0.2 mM NADH, 1 mM phosphoenolpyruvate, 3.5 units of pyruvate kinase, and 5 units of lactate dehydrogenase. In a parallel experiment, Mtr4p was incubated with varying amounts of RNA (0 - 4 μM) and 4 mM ATP under the same conditions as described above. Oxidation of NADH to NAD+, which is coupled to ATP hydrolysis, was continuously monitored at 338 nm in a Beckman DU-640 spectrophotometer. Initial rates were calculated from the change in absorbance using a net extinction coefficient (Δε338) of −6220 M−1cm−1 (reflecting the fact that the conversion of NADH to NAD+ decreases absorbance at 338 nm). As a control, the absorbance change as a function of time for samples omitting ATP or RNA, depending on the experiment, was subtracted from the initial rate at each ATP or RNA concentration. Kinetic parameters were determined by fitting the rates as a function of ATP or RNA concentration to the Michaelis-Menten equation using the KaleidaGraph software package (Synergy Software). The lack of detectable ATP hydrolysis in the presence of R20 for either of two ATPase-deficient Mtr4p mutants (K177A and D262A) confirms that contaminating ATPases do not interfere with these experiments (data not shown).
To determine the kinetic parameters for release of each of the four Mtr4p 20 nt substrate complexes (Table 1), we incubated a fixed amount of protein (150 nM) with fluorescein-labeled ssRNA and measured the decrease in anisotropy as a function of time. Dissociation of the Mtr4p-RNA complex was stimulated by a competitive challenge with 5000-fold molar excess unlabeled ssRNA of the same sequence. The solution conditions were identical to those employed in the binding affinity experiments. The polarimeter was operated in kinetic mode using a single sample containing all components except the RNAs as a blank. At the initial time point the sample contained all components, except the unlabeled competitor RNA. The unlabeled ssRNA was then added and measurements were taken every 15 seconds for at least 150 seconds. The total fluorescence emission intensity was monitored concurrently with anisotropy to ensure that photobleaching of the fluorescein did not affect the observations. Total fluorescence intensity at the end of each kinetic trace was typically within 5% of the starting value (not shown). The kinetics of complex dissociation was measured for each of the substrates either in the absence of nucleotide, in the presence of AMP-PNP, or in the presence of ATP. The time-dependent decrease in anisotropy was fit to a single exponential equation (where appropriate):
where A is the measured anisotropy at time t, A0 is the amplitude of the reaction at the beginning of the dissociation event, k is the rate of complex dissociation, t is time and B is the minimum anisotropy (i.e., the plateau of the reaction). The initial anisotropy is equal to A0 + B. This binding model assumes that only one dissociation event is taking place. The appropriateness of the single exponential model was evaluated by the agreement between the observed and calculated kinetic traces as determined by a residual runs test. In cases where the single exponential equation was deemed inappropriate, isotherms were analyzed by a two component exponential equation:
where A is the measured anisotropy at time t, A0 is the amplitude of the fast phase of dissociation event, A1 is the estimated amplitude of the slow phase of dissociation, k1 is the rate of the faster dissociation event, k2 is the rate of the slower dissociation event, t is the time, and B is the minimum anisotropy. The initial anisotropy is equal to A0 + A1 + B.
Mtr4p binds RNA with a clear preference for short poly(A) tracts (19). However, the basis for this preference is not well-understood. Polyadenylation via the TRAMP complex is a necessary signal that promotes exosome-mediated RNA processing. Thus, understanding the properties that give rise to preferential binding to poly(A) will shed light on how key substrates are selected and targeted for processing by the exosome. We employed MBDA to examine the differences between Mtr4p-RNA complexes more explicitly. The change in Mtr4p binding density (Σν, or number of proteins bound per RNA) yields important insights into how ATP and sequence-specific RNA interactions affect the Mtr4p-RNA complex architecture and hence how substrates are selected. In addition, the magnitude of observed signal as a function of binding density yields information about the nature of structural changes that accompany complex formation. In addition, MBDA can identify the number of distinct binding modes for a given Mtr4p-RNA complex. The Mtr4p binding density (Σν) was measured using fluorescence anisotropy in the presence of three different concentrations of RNA for each condition (i.e. A20 and R20; nucleotide-free, ADP-bound, and AMP-PNP-bound for both substrates). These three binding isotherms were analyzed by MBDA to assess complex behavior and to determine the number of nucleotides Mtr4p occludes upon binding to a particular substrate in a given nucleotide-bound state. The non-linear nature of the change in anisotropy as a function of binding density indicates that these Mtr4p titrations exhibit at least two binding modes for both the A20 and R20 substrates, a low binding density mode and a high binding density mode. The stoichiometry of the low binding density mode was determined as follows. The Mtr4p-dependent change in fluorescence anisotropy (ΔA) was calculated as a function of the average number of Mtr4p molecules bound per RNA strand (Σν) as described (33). Tangent lines to slopes corresponding to low and high density phases of the isotherm (45) were then calculated. The intersection of the two phases was taken as the stoichiometry of the low binding density mode (45). From the stoichiometry and the assumption that there is only one RNA strand bound by a given Mtr4p protein, the site size is simply calculated as (N/ενi), where N is the number of nucleotides in the substrate, and ενi is the binding density for complex i. Saturation of RNA with Mtr4p requires very high protein concentrations and varies little with substrate or nucleotide. Therefore, we focused on the low binding density mode to determine thermodynamic differences between substrates and nucleotide-bound state.
For the Mtr4p-R20 complex, the site size of the low binding density mode increased markedly as a function of nucleotide-bound state: from 5.3 ± 1.0 nt in the nucleotide-free complex, to 6.8 ± 1.9 nt in the ADP-bound complex, and finally to 16.7 ± 2.9 nt in the AMP-PNP-bound complex (Table 2). However, the overall architecture of the complex, as judged from the curvature of the ΔA versus ΣνI plots (Figure 1A), does not appear to change significantly. The Mtr4p-R20 complex exhibits a steep anisotropy dependence on Σν for the low binding density mode and a more modest increase for the high binding density mode, regardless of nucleotide-bound state. This suggests that the primary difference between the nucleotide-free and AMP-PNP-bound complexes is an expansion of the contact surface of RNA occluded by Mtr4p.
In contrast, the site size of the Mtr4p-A20 complex in the low binding density mode does not vary appreciably from 5 nt, regardless of nucleotide-bound state (Table 2). The architecture of the Mtr4p-A20 complex, however, appears to change radically upon binding AMP-PNP. This is evident from the dependence of anisotropy change on binding density for the Mtr4p-A20 versus Mtr4p-A20-AMP-PNP complexes (Figure 1B). For the Mtr4p-A20 complex in the low binding density mode, the change in anisotropy with increasing binding density is steep, as would be expected for a complex between a 123 kDa protein (Mtr4p) and a 6 kDa substrate (A20). The increase in anisotropy with increasing binding density is comparatively modest in the high binding density mode. Strikingly, for the Mtr4p-A20-AMP-PNP complex in the low binding density mode, a shallow increase in anisotropy is observed. After the transition to the high binding density mode occurs, the anisotropy increases sharply. The steep slope of the high binding density mode of the Mtr4p-A20-AMP-PNP complex suggests that this complex undergoes significant conformational remodeling at higher binding densities. Further, based on the behavior of the low binding density modes, these complexes appear to have distinct architectures at lower binding densities as well.
Presumably, the conformational change in Mtr4p caused by binding of AMP-PNP is similar in the presence of both substrates. Therefore, the ability to induce such different changes in architecture upon binding to either the Mtr4p-R20 or the Mtr4p-A20 complex is noteworthy. These data indicate that conformational changes of the Mtr4p-RNA complex created by binding of ATP are substrate specific. The distinct binding mode and architecture of the poly(A) complex likely reflects the underlying mechanism whereby Mtr4p can distinguish poly(A) from other sequences.
Changes in binding affinity as a function of RNA sequence, RNA structure, and nucleotide-bound state provide details regarding the conditions which favor targeting to the exosome and Mtr4p-assisted RNA processing. Previous studies clearly showed the following: Mtr4p prefers to bind free 3′-ends, Mtr4p prefers poly(A) substrates to those of random sequences, and nucleotide binding generally decreases Mtr4p affinity for RNA substrates (19). In these studies, we sought to determine if the trends for poly(A) versus random substrates extended to other repetitive sequences, namely poly(U) and poly(UC). Thus, we determined the affinity of Mtr4p for the four 20 nt substrates shown in Table 1 by fluorescence anisotropy (Table 3 and (19)). From these data, several trends emerge. In particular, Mtr4p exhibits apparent cooperative binding behavior for both the homopolymers (i.e. A20 and U20), and the (UC)10 repeating sequence. In our previous studies, we observed two bound species in electrophoretic mobility shift assays (EMSAs) for the A20 substrate independent of nucleotide-bound status (19), and statistical analyses of model fits to the binding isotherms clearly showed that a single site model was inappropriate. Despite the clear presence of two bound species in the EMSA, the two binding events could not be resolved from anisotropy isotherms. Thus, we used a transformed Hill model (Equation 6) to fit the observed change in anisotropy as a function of Mtr4p concentration (19). With the U20 and (UC)10 substrates, statistical analyses of model fits also showed that the transformed Hill model was appropriate. A second feature of these binding isotherms is that nucleotide binding modulates the affinity of the Mtr4p-R20 complex differently than the other complexes. For the Mtr4p-R20 complex, the AMP-PNP-bound species clearly is the lowest affinity complex. The Mtr4p affinity for the R20 substrate in the presence of ADP was statistically indistinguishable (p value 0.48) from that in the absence of nucleotide. In contrast, for the other 20 nt Mtr4p-substrate complexes, the ADP-bound species is the lowest affinity complex. Other subtle trends are also evident. For the A20 and U20 substrates, the nucleotide-free species is clearly the highest affinity complex, whereas for the (UC)10 substrate, the AMP-PNP-bound species is the highest affinity complex. This behavior might reflect the affinity for ATP rather than the (UC)10 substrate if the tight binding of RNA in the presence of AMP-PNP reflects a lack of affinity for the nucleotide itself. This idea is supported by the poor Mtr4p ATPase activity when presented with the (UC)10 substrate (Table 4 and below). Because differences in solution salt conditions can influence binding properties, we tested the affinity of Mtr4p for both the A20 and R20 substrates in the absence of nucleotide under near physiological salt conditions. The salt concentration increase from 50 mM to 90 mM univalent salt and from 0 to 1 mM Mg2+ significantly weakened the binding to both substrates (data not shown), but the preferential binding of Mtr4p to the A20 substrate was maintained in both solution conditions. Thus, we standardized our assay using the lower ionic strength conditions because the data quality is significantly improved over that collected with physiological salt concentrations. In general, for substrates as long as 20 nt, sequence content appears to have only a modest effect on the affinity of Mtr4p for a given substrate. However, both the mode of interaction (i.e., presence of apparent cooperative behavior) and regulation by nucleotide binding differ for random-sequenced substrates versus substrates containing repetitive sequences.
Sequence content alone is not likely to be the only parameter that affects nucleotide-dependent changes in the affinity of Mtr4p for a given substrate. Substrate length is apt to have a large influence. In the various RNA processing and degradation pathways, Mtr4p acts in concert with the exosome, which truncates substrates by exonucleolytic cleavage. Thus, the ability of Mtr4p to bind shorter ssRNA stretches will significantly impact the ability of Mtr4p to deliver RNAs and assist the exosome in processing substrates containing those sequences at their 3′-end. To examine the ability of Mtr4p to bind short oligonucleotides and to provide an orthogonal examination of Mtr4p site size requirements for comparison with the MBDA described above, we used poly(A) and random-sequenced substrates of 10 and 5 nucleotides in length (i.e. A10, A5, R10, and R5). Based on the MBDA analysis, truncating the R20 substrate to 10 nucleotides would result in a substrate with two binding sites in the absence of nucleotide, one binding site in the presence of ADP, and less than one binding site in the presence of AMP-PNP. For the Mtr4p-poly(A) complexes, truncating the length to 10 nucleotides would remove two binding sites in all nucleotide-bound states. When the R20 substrate is reduced to R10 in the absence of nucleotide, we observed a two-fold decrease in affinity. Strikingly, the affinity in the presence of ADP decreases by approximately 33-fold, and the presence of AMP-PNP causes approximately a 12-fold decrease in affinity (Table 3). It is clear that removal of up to two binding sites decreases Mtr4p affinity for random-sequenced substrates in the absence of nucleotide. For the R10-ADP complex, the loss of binding sites resulting from an increased site size (7 nt) causes a much more profound loss of affinity. Similarly, the Mtr4p-R10-AMP-PNP complex, for which the site size is 17 nt, is a low affinity complex. It is possible that the presence of bound nucleotide enhances the effect of losing binding sites in the ADP- and AMP-PNP-bound forms. However, the site size of the Mtr4p-R20 complex changes significantly upon nucleotide binding, making it difficult to separate the effects of changes in the number of available binding sites from a site size-independent change in affinity caused by nucleotide binding. Reducing the length of the A20 substrate to 10 nucleotides did not cause a shift to single-site binding behavior for any of the nucleotide-bound states. This behavior agrees well with a calculated intersection site size of 5 nt (independent of nucleotide-bound status) as determined by MBDA. In the presence of AMP-PNP, the affinity of Mtr4p for A10 is weak, and we therefore cannot confidently distinguish between the single-site and modified Hill binding models. Despite the fact that approximately two binding sites remained for all nucleotide-bound states, we observed that the affinity of Mtr4p for A10 was less for each of those states than that observed for A20, most likely due to the loss of cooperative interactions that promote high-affinity binding. In the absence of nucleotide, a two-fold decrease in affinity was observed. The addition of nucleotide caused a further decrease in affinity, approximately 3-fold in the presence of ADP and approximately 10-fold in the presence of AMP-PNP (Figure 2). Unlike the random-sequenced substrate, because the site size of Mtr4p on poly(A) does not change significantly upon nucleotide binding, we can assess the contributions of losing binding sites and nucleotide binding to changes in affinity. It is clear that the loss of up to two binding sites on the poly(A) substrate decreases affinity for that substrate (this change is similar in magnitude to that observed when R20 is truncated to R10 in the absence of nucleotide). In addition to the effect of removing binding sites, there appears to be an intrinsic loss of affinity induced by nucleotide binding that favors Mtr4p binding to longer poly(A) tracts (i.e., the penalty for truncating from 20 to 10 adenylates is greater in both the ADP- and AMP-PNP-bound states than in the absence of nucleotide). This is similar to our previous observation that a loss of affinity upon nucleotide binding can allow Mtr4p to discriminate 3′-tailed substrates from 5′-tailed substrates (19). Furthermore, because more than one binding site and thus the opportunity for cooperative interactions remains, binding of Mtr4p to the A10 substrate is tighter in all nucleotide-bound states than for the R10 substrate.
Truncation to 5 nucleotides would leave at most a single binding site for any of the Mtr4p-substrate-nucleotide complexes. We observed that such truncation causes a significant decrease in affinity in the absence of nucleotide for both substrates. In the absence of nucleotide, the R5 substrate contains a single binding site, resulting in an additional approximately 30-fold reduction in affinity relative to the R10 substrate (Figure 2). For the A5 substrate in the absence of nucleotide, the presence of a single binding site results in an additional approximately 6-fold decrease in affinity relative to the A10 substrate and single-site binding behavior. Therefore, the poly(A) and random oligomer truncation studies are consistent with MBDA predictions for both substrates in the nucleotide-free complex. The presence of either ADP or AMP-PNP caused the affinity to decrease to Kd > 2 μM for both the A5 and R5 substrates. It is intriguing that the binding site size of the Mtr4p-R20-AMP-PNP complex is 17 nt, yet Mtr4p is able to bind the R10 and R5 substrates. It is possible that Mtr4p binds R10 and R5 in a mode that is distinct from that of R20 under certain conditions (i.e., nucleotide-bound, high protein concentration). Further, binding of Mtr4p to these shorter substrates is likely dependent on saturation binding, which occurs at high protein concentrations and might have less physiological relevance. These data indicate that a single binding site is a poorly-interacting substrate. However, for a single binding site in the absence of bound nucleotide, a random-sequenced substrate has a markedly lower baseline affinity than a poly(A) substrate.
These results show that as the number of binding sites available for Mtr4p to bind decreases, the affinity of Mtr4p for that substrate also decreases. In addition, due to the observed apparent cooperative behavior, Mtr4p binds to the 10 nt truncated poly(A) substrates with higher affinity than their random-sequenced counterparts in all nucleotide-bound states. The loss of affinity upon truncation of the poly(A) substrates is exacerbated when either ADP or AMP-PNP is bound, whereas the effect of nucleotide binding to the truncated random-sequenced substrates is less well-defined. This indicates that the mechanism by which Mtr4p is able to discriminate substrates derives from a combination of the number of available binding sites and the effect of nucleotide binding on both affinity and site size. Such a mechanism allows Mtr4p to effectively distinguish poly(A) from random substrates independent of nucleotide-bound status.
Efficient hydrolysis of ATP is a requirement for any helicase, and Mtr4p possesses RNA dependent ATPase activity (16, 19). The ability of Mtr4p to hydrolyze ATP in response to substrate-specific interactions is likely to have a significant impact on both substrate delivery and the efficiency of Mtr4p-exosome mediated processing. The ability of Mtr4p to hydrolyze ATP in the presence of the model substrates in Table 1 was assayed spectrophotometrically using a coupled enzyme assay. We found the sequence of the RNA substrate to have a profound effect on the Michaelis-Menten parameters of ATP hydrolysis. The Mtr4p-R20 complex is the most efficient ATPase. This is clear from the observed Km (0.1 mM), kcat (444 min−1), and kmax (519 min−1). Each of these parameters shows R20 to be at least 3-fold more efficient as a stimulator of Mtr4p ATPase activity than any other substrate tested (Figure 3 and Table 4). Unlike the other kinetic parameters, the Kapp(RNA) for R20 (179 nM) is comparable to both the A20 (211 nM) and U20 (193 nM) substrates, indicating that affinity for the RNA substrate does not account for differences in catalytic rate. To ensure that the enzyme kinetic parameters determined were not significantly influenced by the experimental conditions, we determined the kcat and Km for the R20 substrate at physiological salt conditions, and at subsaturating RNA levels. Changing the buffer system to physiological salt had no effect on either kcat or Km (data not shown). At subsaturating RNA, the Km was statistically indistinguishable, (p value 0.17) from the saturated RNA conditions, and the kcat was significantly reduced as expected (data not shown). The A20 and U20 substrates stimulate ATPase activity to a very similar degree. In fact, all of the kinetic parameters are statistically indistinguishable for the two substrates (Table 4). Despite the ability of Mtr4p to bind to (UC)10, that substrate could not stimulate ATP hydrolysis. We observed measurable catalysis but the rates determined were unreliable and very weak. For all of the substrates tested, the Kapp values were significantly larger than the estimated affinity based on direct binding to the substrate in the presence of AMP-PNP (Table 3). These differences imply that the apparent binding constants include contributions from some other kinetically relevant event. The nature of the assay (i.e. substrate affinity is measured indirectly) precludes determination of which event is the source of this discrepancy.
Mtr4p, as part of its function in nuclear RNA processing, will encounter substrates truncated by the exosome. The manner in which Mtr4p responds to substrates that have been or are being truncated will in part determine which substrates can or cannot be processed. To examine the effect of substrate truncation on ATP hydrolysis, we determined the ATPase kinetic parameters for truncated random-sequenced and poly(A) substrates. As we found in the binding affinity studies above, RNA substrate truncation differentially affects Mtr4p ATP hydrolysis kinetics in the presence of random versus poly(A) substrates (Figure 3 and Table 4). Truncation of R20 to R10 decreases both the rates of ATP hydrolysis (kcat and kmax, approximately 3-fold) and the affinity for both ATP and RNA (Km and Kapp, 6-10 fold). For the R20 and R10 substrates kcat = kmax indicating that the same Mtr4p-ATP-RNA complex forms prior to catalysis, regardless of whether saturation is reached for Mtr4p-ATP or Mtr4p-RNA (46). This is not the case for the R5 substrate (below). In contrast, truncation of A20 to A10 had no effect on kcat and kmax, but a severe effect on Km (13-fold decrease) and Kapp (2.4-fold decrease). Surprisingly, upon truncation of the R10 substrate to R5, neither Km nor Kapp is appreciably affected, whereas kcat and kmax both decrease. Truncation of A10 to A5 completely abolished the ability to stimulate Mtr4p ATP hydrolysis, despite 10-fold higher affinity of A5 relative to R5 in the direct binding assay (in the absence of nucleotide, Table 3). This effect is probably due to a further decrease in the affinity of Mtr4p for ATP in the presence of the A5 substrate. Since the Km in the presence of A10 is 5.2 mM, any further decrease in affinity for ATP could conceivably abolish ATPase activity. These data indicate that decreasing the length of R20 can negatively impact both the apparent affinity for ATP and RNA, and the chemical steps that facilitate ATP hydrolysis. In contrast, truncating a poly(A) substrate causes a loss of affinity for ATP and RNA while the chemical processes involved in the hydrolysis of ATP are unaffected. In general, upon truncation of random-sequenced substrates, Mtr4p has significantly higher affinity for ATP but weaker apparent affinity for RNA substrates. Importantly, a random-sequenced substrate containing a maximum of one binding site can stimulate Mtr4p ATP hydrolysis, whereas a poly(A) substrate requires more than one binding site to stimulate Mtr4p ATP hydrolysis. Taken together, these data show that homopolymeric substrates attenuate the ATPase activity of Mtr4p relative to random-sequenced substrates, most likely due to decreased affinity for ATP. These data further confirm that the interactions between random-sequenced and poly(A) substrates are fundamentally distinct and therefore those substrates are likely to be processed differently by the Mtr4p-exosome system.
One potential role of Mtr4p is targeting substrates to the exosome. A natural requirement for targeting is that the Mtr4p-substrate complex remains intact. Therefore, substrates containing RNA sequence motifs that promote slowly dissociating Mtr4p-RNA complexes are more likely to be targeted to the exosome. Conversely, RNA substrates that contain sequence motifs which promote quickly dissociating Mtr4p-RNA complexes are likely to influence its catalytic cycle by promoting turnover of Mtr4p. The kinetics of dissociation describes the point at which Mtr4p ATP hydrolysis promotes RNA structure modification through movement and/or enzyme recycling. Such recycling might be required for activity. The rate(s) of dissociation of an Mtr4p-RNA complex was determined by measuring the decrease in anisotropy as a function of time in the presence of the four 20 nucleotide RNA sequences shown in Table 1. Unlabeled oligonucleotides are effective competitors for Mtr4p binding since the apparent inhibition constants (Ki,app) of each unlabeled oligonucleotide obtained via competition experiments were similar to measured affinities in direct binding experiments ( (19) and data not shown). The decrease in anisotropy of the Mtr4p-RNA complex was analyzed using either a single or a double exponential equation. The fits of the two model equations were compared using an F-test to determine the appropriate model. We took a p value of <0.05 to indicate that the double exponential provided a statistically significant improvement to the fit of the data. We have found that both substrate sequence and nucleotide binding can give rise to biphasic dissociation kinetics, yielding dissociation rates for a fast (k1) and a slow (k2) dissociating population. We first used this analysis to better describe the dissociation of the A20 and R20 substrates from Mtr4p, for which we had previously reported estimated half-lives based on a single exponential fit (19); indicated by an asterisk in Table 5). The Mtr4p-R20 nucleotide-free complex has rapid but measurable dissociation kinetics and a single dissociating species with a rate of dissociation (k1) of 0.046 s−1, which corresponds to a half-life (t1/2) of 15 s. Interestingly, the presence of AMP-PNP confers a second Mtr4p-R20 dissociating population (p value <0.004). The major population has a faster k1 (0.077 s−1, t1/2 = 9 s) than the nucleotide-free complex and encompasses approximately 82% of the total decrease in anisotropy (Figure 4). As the population of the second dissociating species contributes only 18% of the observed anisotropy decrease, the net result is a similar aggregate rate of dissociation to the nucleotide-free complex. The Mtr4p-A20 complex is much less dynamic and is characterized by the presence of at least two dissociating species both in the absence of nucleotide and in the AMP-PNP bound complex. In the nucleotide-free Mtr4p-A20 complex, we detect two dissociating species, with the slower dissociating species (k2 = 0.0036 s−1, t1/2 = 204 s) contributing 61% to the overall decrease in anisotropy (Figure 4). We also detect two dissociating populations in the Mtr4p-A20-AMP-PNP complex, but for that complex both k1 and k2 are faster, and k1 dominates rather than k2, yielding a faster overall rate of dissociation. This pattern does not appear to arise due to the homopolymeric nature of poly(A), as the Mtr4p-U20 complex dissociates very rapidly in its nucleotide-free form (k1 > 0.13 s−1, t1/2 < 5 s). The Mtr4p-U20-AMP-PNP complex, like the equivalent R20 complex, contains a second, long-lived dissociating species. However, unlike the other complexes, AMP-PNP binding actually retards dissociation of the Mtr4p-U20-AMP-PNP complex relative to the nucleotide-free form. The Mtr4p-(UC)10 complex is extremely dynamic regardless of nucleotide presence. The Mtr4p-(UC)10 complex has a single dissociating species in all cases with a k of > 0.13 s−1 (Figure 4). For each substrate, we examined the rate of dissociation in the absence of nucleotide under physiological salt conditions to ensure that the ionic strength of our experimental conditions did not alter the trends we observed (data not shown).
We also examined dissociation kinetics in the presence of ATP. The conditions of this assay are nearly identical to those in which we conduct our ATPase assay, indicating that Mtr4p is hydrolyzing ATP during the course of the dissociation kinetics experiment. As expected, in the presence of ATP, the Mtr4p-R20 and Mtr4p-A20 complexes are much more dynamic, and contain a single observable dissociating species, suggesting that ATP hydrolysis, and not just ATP binding induces the release of the substrate (Table 5). However, under conditions of ATP hydrolysis, the dissociation rate of the R20 complex (k1 > 0.13 s−1, t1/2 <5 s) is significantly faster than that of the A20 complex (k1 = 0.046 s−1, t1/2 = 15 s). Strikingly, the formation of the Mtr4p-U20-ATP complex severely retards complex dissociation. Further, the Mtr4p-U20-ATP and Mtr4p-U20-AMP-PNP complexes contain two dissociating species with nearly equal rates of dissociation but for which the amount that each species contributes to the overall rate of dissociation is markedly different for ATP and AMP-PNP. In the presence of AMP-PNP nearly 70% of the population is in the faster dissociating species (k1 > 0.13 s−1, t1/2 <5 s). The Mtr4p-U20-ATP complex favors the k2 state (0.0029 s−1, t1/2 = 171 s; this population encompasses approximately 82% of the total decrease in anisotropy amplitude). Thus, both ATP binding and to a much greater extent ATP hydrolysis inhibit the dissociation of Mtr4p from poly(U) substrates whereas ATP hydrolysis clearly accelerates dissociation from the R20 and A20 substrates. Based on these data, we conclude that each of the Mtr4p-RNA complexes (with and without nucleotide) studied here has unique, sequence specific interactions with Mtr4p, which generates a particular dissociation kinetic profile for each species. Most importantly, there must be a distinct interaction with poly(A) that slows Mtr4p dissociation relative to the random-sequenced substrate independent of nucleotide binding or hydrolysis.
The mechanism whereby Mtr4p interacts with its substrates has a great impact on all its functions: helicase activity; ATPase activity; and the putative targeting function. All three of these functions are no doubt intimately related as part of the coordination of Mtr4p activity with degradation by the exonucleolytic exosome complex. While both the addition of short 3′ poly(A) tails and the degradation of substrates containing those tails have been well documented, the pathway from polyadenylation to eventual degradation remains undefined. Polyadenylation is an energetic investment the cell makes in order to ensure timely degradation or processing of a given substrate. One way to guarantee that the investment will produce the desired outcome is to directly target the polyadenylated substrate to the degradation machinery. There is precedent for such targeting in RNA processing. Mammalian AU-rich element (ARE) binding proteins direct substrates to the cytoplasmic exosome for exonucleolytic decay (47). Likewise, the Schizosaccharomyces pombe (S. pombe) poly(A)-binding protein 2 (Pab2) can target some polyadenylated snoRNAs to the S. pombe exosome (48). In order for targeting to occur, the protein-RNA complex formed must possess properties that make encounters with the degradation machinery more likely. The data we report here shows that S. cerevisiae Mtr4p, which is both a poly(A)-binding protein like S. pombe Pab2 and a helicase, forms a complex with poly(A) RNA that is ideally suited for targeting to the exosome. In particular, the Mtr4p-poly(A) complex promotes cooperative interactions that drive high-affinity binding, is comparatively resistant to truncation, and possesses an attenuated propensity to dissociate either in response to competing RNA substrates or ATP hydrolysis. Many substrates encountered by Mtr4p in vivo will be of mixed sequence, with stretches of poly(A) and random or U-rich regions. Based on our data, it is likely that the behavior of such a complex will depend on the length of the poly(A) tract and the length of the sequence located 5′ of the poly(A) tract. We anticipate that a substrate with more than 10 adenylates at the 3′-end will behave largely like the poly(A) model substrate described here. As a caveat, an A-rich region within the interior of a substrate may exhibit different behavior than that observed for a poly(A) 3′-end. It is also possible that an extended (i.e. 10-20 or more adenylates) poly(A) tract at the 3′-end of a substrate could form a complex in which Mtr4p proteins bound to the poly(A) region tether another Mtr4p protein (or proteins) to a 5′ stretch of random sequence adjacent to, e.g., an element of secondary structure.
Based on the MBDA analysis, one can distill the poly(A) and random substrates down to a minimal site of ≈ 5 nucleotides. In agreement with our results, a recent crystal structure of a Mtr4p-A10-ADP complex (22) confirms that in its main interaction mode with poly(A) Mtr4p contacts 5 nucleotides. For that minimal site, Mtr4p binds poly(A) approximately 10-fold more tightly than the random-sequenced substrate. Thus, at any given time there will be many more Mtr4p-short poly(A) complexes than similar complexes with random-sequenced substrates, thereby increasing the likelihood of Mtr4p-poly(A) complexes encountering other RNA processing factors. Such a property could play an important role in promoting multiple rounds of polyadenylation and degradation as might be required for highly-structured substrates (12). For example, given the preference of Mtr4p for poly(A), delivery of a substrate to the Trf/Air polyadenylation complexes should increase in frequency if, for example, the substrate has already undergone limited polyadenylation and/or partial degradation. Since most of the Mtr4p present in the cell exists outside the TRAMP complex (11), one role of Mtr4p could be to recruit the Trf/Air polyadenylation complexes to partially adenylated substrates to ensure the creation of a footprint sufficient to foster degradation by the exosome. Nucleotide binding markedly decreases the affinity of Mtr4p for the A5 substrate, suggesting that ATP-binding can be an effective regulator of poly(A) selection. As the number of binding sites increases, the differences in affinity between the poly(A) and random-sequenced substrates (and the poly(U) and poly(UC) substrates) become smaller; however, Mtr4p can still discriminate RNA substrates because other characteristics of the complexes still differ markedly. The basis for discrimination most likely lies in the large differences in architecture of the Mtr4p-poly(A) complexes relative to the complexes with random-sequenced substrates, and changes in the architecture of the Mtr4p-poly(A) complexes in response to nucleotide binding and hydrolysis. Comparison of the apo and Mtr4p-A10-ADP structures shows significant structural shifts, particularly in domains 2 and 4, which contact the bound RNA (not shown). These shifts are consistent with the Mtr4p-ssRNA complex architectural changes suggested by our MBDA analysis. While it is possible that the KOW domain of Mtr4p stabilizes some substrate complexes, all available data suggests that this happens at high protein concentrations (22), far beyond that required to saturateMtr4p binding with our model substrates. Moreover, while it is likely that the KOW domain may contribute to binding some substrates, other contacts appear make more important contributions to binding affinity. In particular, the 3′-end of the A10 substrate in the co-crystal abuts the interface between domains 1 and 4, with interactions between R272 and O4′ of the 3′-ribose and between R1030 and the exocyclic amino group of the 3′ adenosine. Adjacent to the 5′-most observed nucleotide, there is a large solvent channel which could easily accommodate the remainder of the A10 substrate. Despite the close proximity of the KOW domain to the region where the 5′-end of the A10 substrate likely resides, no contacts between the two are evident. However, with larger substrates, or perhaps in different nucleotide-bound states, the KOW domain could, either by nature of this proximity or nucleotide-induced conformational rearrangement, productively interact with a bound RNA substrate.
Our studies of the kinetics of ATP hydrolysis and Mtr4p-RNA complex dissociation show suppression of both activity and complex dissolution consistent with the putative targeting function. The efficiency of targeting a given substrate to the exosome machinery will depend in part on how long that substrate stays bound to the protein that does the targeting. In turn, nucleotide binding and hydrolysis can have a large effect on the stability of the Mtr4p-RNA complex. We observe that the homopolymeric A20 and U20 substrates are much less efficient stimulators of Mtr4p ATP hydrolysis than the R20 substrate (Table 4). The difference in efficiency is particularly striking for the single binding site (A5 and R5) substrates. The R5 substrate can stimulate Mtr4p ATPase activity, with a catalytic rate (101 ± 5 min−1) that is statistically indistinguishable from the A20 substrate (124 ± 18 min−1; however, the affinity for both ATP and RNA are far weaker for the R5 substrate than the A20 substrate, see Table 4). These differences in ATPase activity are not likely due to effects of RNA secondary structure. While the R20 substrate might form transient secondary structures during the time course of our experiment, the R5 substrate most certainly cannot form such structures. Therefore, the attenuated ATPase activity observed for the A20 and U20 substrates arises due to a fundamental difference in the way Mtr4p interacts with these substrates relative to the random-sequenced substrate. Furthermore, the steady-state cellular ATP concentration in yeast is approximately 4 to 8 mM (49) and can vary significantly depending on growth conditions (50). If the nuclear/nucleolar concentration of free ATP falls within the same range and the RNA substrate concentration is saturating, then we would expect the response of Mtr4p-substrate complexes in vivo to ATP to vary considerably with substrate sequence. In particular, for complexes with random-sequenced 3′-tails as short as 5 nt, Mtr4p should be able to hydrolyze ATP with at least moderate efficiency because ATP is likely to be saturating for those complexes. In contrast, this amount of ATP will likely be subsaturating for a poly(A) tail as long as 10 nt and therefore ATP hydrolysis is expected to be comparatively inefficient. In conjunction with suppressed ATPase activity, we observe a marked decrease in the rate of dissociation for the A20 substrate relative to the R20 substrate. When compared with the other substrates, the Mtr4p-A20 complex is the least dynamic (Figure 4D). These data suggest that, in the absence of nucleotide, poly(A) tailed substrates would dissociate slowly, allowing the RNA to be targeted to the exosome. The presence of AMP-PNP increases the dynamics of both the Mtr4p-A20 and Mtr4p-R20 complexes relative to the absence of nucleotide. In the presence of ATP, the Mtr4p-A20 and Mtr4p-R20 complexes are much more dynamic, suggesting that ATP hydrolysis, and not just ATP binding, induces the release of the substrate (Table 5). However, in the presence of ATP, release of the substrate is still markedly slower for the A20 substrate than for the R20 substrate. These data show that, regardless of nucleotide-bound state the Mtr4p-poly(A) substrate complex is less likely to dissociate than the Mtr4p complex with a random-sequenced substrate, thus providing a greater window of opportunity for Mtr4p to deliver the poly(A) substrate to the exosome. Further, the rate of dissociation of the Mtr4p-R20-ATP complex indicates that Mtr4p, absent a functional tether (e.g. the exosome), will rapidly release a random-sequenced substrate upon hydrolysis of ATP.
Curiously, the Mtr4p-U20 complexes show the opposite trend in dissociation kinetics relative to Mtr4p-A20 complexes. The Mtr4p-U20 association is highly dynamic in the absence of nucleotide (t1/2 < 5 s). Upon binding AMP-PNP, the complex becomes less dynamic. The Mtr4p-U20-ATP complex is the least dynamic complex of the three. Under our experimental conditions, active ATP hydrolysis should proceed during the dissociation kinetics experiment. This suggests that ATP hydrolysis impedes dissociation. The significance of this observation is unknown, but it is possible that under certain circumstances Mtr4p might be able to target U-rich substrates to the Trf/Air polyadenylation complexes or the exosome.
In addition to substrate targeting, the rate of complex dissociation as a function of nucleotide binding and hydrolysis is likely to have an impact on both ATPase and RNA structure remodeling activities of Mtr4p. For the DEAD-box helicases, a study in which progression through the ATP hydrolysis cycle was blocked via the use of non-hydrolyzable analogues showed that one function of ATP hydrolysis is to allow enzyme recycling and multiple substrate turnovers that enhance the rate of unwinding (51). Most importantly, the authors demonstrated that ATP hydrolysis stimulates enzyme dissociation as part of the recycling process. Because we also observe that the rate of dissociation for both the A20 and R20 substrates increases significantly in the presence of ATP (Figure 4), it is likely that such rapid substrate release is an integral feature of the catalytic activity of Mtr4p. In fact, the R20 substrate exhibits both the most rapid dissociation kinetics in the presence of ATP and the most robust stimulation of Mtr4p ATPase activity.
In summary, we view targeting as a stochastic process which reflects the increased likelihood that a given protein-RNA complex will encounter the degradation machinery. Each of the unique features of the Mtr4p-poly(A) complex that we observe (i.e. increased affinity, suppressed ATP hydrolysis, decreased rate of dissociation) stem from the unique binding mechanism used by Mtr4p to interact with poly(A). Each feature alone could increase the likelihood that an Mtr4p-poly(A) complex will encounter RNA processing factors relative to other substrates. In sum, these features are likely to markedly increase the efficiency with which polyadenylated substrates are targeted to either the polyadenylation or degradation machinery.
The authors would like to thank Dr. Laura Mizoue of the Center for Structural Biology at Vanderbilt University for providing the expression plasmid used in these studies. The authors also acknowledge the assistance of Paz J. Luncsford with several control experiments.
†This work was supported funds from the Marlene and Stewart Greenebaum Cancer Center (EAT) and National Institutes of Health grant R01 CA102428 (GMW).
1The abbreviations used are: Fl, fluorescein; EMSA, electrophoretic mobility shift assay; ss, single-stranded; ds, double-stranded; nt, nucleotide; AMP-PNP, Adenosine 5′-(β,γ-imido)triphosphate; ADP, Adenosine 5′-diphosphate; rRNA, ribosomal RNA; mRNA, messenger RNA; tRNA, transfer RNA; CUT, cryptic unstable transcript; S. pombe, Schizosaccharomyces pombe; S. cerevisiae, Saccharomyces cerevisiae