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Induction of Positive Cooperativity by Amino Acid Replacements Within the C-

Terminal Domain of P. chrysogenum ATP Sulfurylase*

Ian J. MacRae‡, Eissa Hanna‡, Joseph D. Ho‡, Andrew J. Fisher§‡, and Irwin H. Segel‡¶

‡Section of Molecular and Cellular Biology and §Department of Chemistry University of California, One Shields Avenue, Davis, CA 95616

Running Title: Positive Cooperativity of ATP Sulfurylase Key Words: Sulfurylase, ATP, kinetics of mutant enzymes; Kinetics, mutant ATP sulfurylases; Allosteric domain, fungal ATP sulfurylase; Cooperativity, induction by site-directed mutagenesis; Mutagenesis, ATP sulfurylase. Correspondence to: I. H. Segel at above address e-mail: ihsegel@ucdavis.edu Telephone: 530-752-3193 FAX: 530-752-3085

Copyright 2000 by The American Society for Biochemistry and Molecular Biology, Inc.

JBC Papers in Press. Published on August 23, 2000 as Manuscript M005992200 by guest on A

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SUMMARY

ATP sulfurylase from Penicillium chrysogenum is an allosteric enzyme in which Cys-509 is critical for maintaining the R state. Cys-509 is located in a C-terminal domain that is 42% identical to the conserved core of APS kinase. This domain is believed to provide the binding site for the allosteric effector, 3’-phosphoadenosine 5’-phosphosulfate (PAPS). Replacement of Cys-509 with either Tyr or Ser destabilizes the R state resulting in an enzyme that is intrinsically cooperative at pH 8 in the absence of PAPS. The kinetics of C509Y resemble those of the wild type enzyme in which Cys-509 has been covalently modified. The kinetics of C509S resemble those of the wild type enzyme in the presence of PAPS. It is likely that the negative charge on the Cys-509 side chain helps to stabilize the R state. Treatment of the enzyme with a low level of trypsin results in cleavage at Lys-527, a residue that lies in a region analogous to a PAPS motif-containing mobile loop of true APS kinase. Both mutant enzymes were cleaved more rapidly than the wild type enzyme suggesting that movement of the mobile loop occurs during the R-T transition.

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(INTRODUCTION) ATP sulfurylase (MgATP: SO42- adenylyltransferase, EC2.7.7.4) catalyzes the first

intracellular reaction in the incorporation of inorganic sulfate into organic molecules by sulfate assimilating organisms:

MgATP + SO42--- MgPPi + APS1

APS is then phosphorylated to PAPS in a reaction catalyzed by the second sulfate-activating enzyme, APS kinase, (MgATP : APS 3’-phosphotransferase, EC 2.7.1.25):

MgATP + APS PAPS + MgADP ATP sulfurylase from the filamentous fungus Penicillium chrysogenum is an oligomer composed of six identical 64 kDa subunits (573 residues). Each subunit possesses three free SH (cysteinyl) groups2, of which, only one (designated SH-1) can be modified by sulfhydryl-reactive reagents such as DTNB and NEM under non-denaturing conditions (1). Complete modification of SH-1 (six per hexamer) changes the initial velocity kinetics at pH 8 from normal-hyperbolic (Hill coefficient, nH = 1) to sigmoidal (nH ca. 2) with a concomitant increase in the [S]0.5 values for MgATP and SO42- (or MoO42---); Vmax,app at a fixed subsaturating cosubstrate level is reduced (2). A number of

experimental approaches, including protection against chemical inactivation by reversibly-bound ligands (2), direct binding measurements (3), and single turnover isotope trapping (3) established that the sigmoidal curves reflected true cooperative binding as opposed to a kinetically-based phenomenon. The dramatic effect of in vitro modification of SH-1 suggested several possible scenarios including that modification induces a conformational state in the enzyme that is normally induced in vivo by a reversibly-bound allosteric effector. The effector was subsequently shown to be PAPS (4). Further experiments established that the enzyme from several other fungi behaved identically to the P. chrysogenum enzyme while ATP sulfurylases from rat liver (5), spinach leaf (6), cabbage leaf (7), yeast (4), and the Riftia bacterial symbiont (8) did not respond in the same way to Cys modification or to PAPS. The cumulative results indicated that (a) fungal ATP sulfurylase possesses an allosteric PAPS binding site that is not present in the enzyme from other sources and (b) SH-1 is either in the region of, or in communication with the PAPS binding site. Fungal sulfurylase was subsequently shown to possess a C-terminal region (residues ca. 396-

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539) that is 42% identical to the conserved core of APS kinase (9 - 11), a protein with a high affinity for PAPS. SH-1 is Cys-509, which is located in the APS kinase-like C-terminal domain, a few residues upstream from a putative PAPS motif (12). It is likely that residue stretch 396 - 540 of P. chrysogenum ATP sulfurylase evolved from true APS kinase and that this region provides the allosteric binding site for PAPS. In effect, the C-terminal region of fungal ATP sulfurylase is a regulatory subunit that happens to be covalently linked to the catalytic subunit3. Our preliminary hypothesis (in terms of the concerted transition model) was that covalent modification of Cys-509 promotes the same R to T allosteric transition (13, 14) as does PAPS binding. The inhibition of P. chrysogenum ATP sulfurylase by PAPS may be the way that fungi prevent PAPS accumulation to toxic levels. Another consideration is that in fungi, PAPS is a major branch point metabolite of sulfate assimilation. One branch leads to cysteine and other reduced sulfur compounds; the other branch to choline-O-sulfate, a sulfur storage compound or/and osmoprotectant (15-18). Thus the inhibition may be part of a more extensive sequential feedback process. In contrast, yeasts and most bacteria do not form large quantities of sulfate esters, while plants (and some bacteria) preferentially use APS (rather than PAPS) as the substrate for the reductive assimilation of sulfate. In other words, PAPS is not at a branch point in these other organisms. The objective of the present study was to establish the role of Cys-509 in stabilizing the R state. To this end, we investigated the kinetic consequences of replacing Cys-509 with either tyrosine or serine.

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MATERIALS AND METHODS

Introducing Mutations. Mutations in codon 509 were made by PCR amplification of the C-terminal 221 base pairs of the fungal ATP sulfurylase gene (codons 506-573). This sequence begins with an indigenous XhoI site three base pairs upstream from codon 509, and ends after the stop codon with an engineered XbaI site. Each PCR used a cloned cDNA copy of the native gene as the template, the C-terminal coding primer PcATS 308 (5'-GGTCTAGATCTTACTGACGCTCCAGGAAACCC-3'), and an upstream primer containing the XhoI site and the desired mutation. Upstream primers with their respective produced mutations were as follows: PcATS315 (C059S), 5'-TCCCCTCGAGCACTCTGAGCAGTCCG-3'; PcATS317 (C509Y), 5'-TCCCCTCGAGCACTACGAGCAGTCCG-3'. All PCRs were carried out using the DNA polymerase Pfu (Stratagene). The resulting 221 bp DNAs were subcloned as XhoI-XbaI fragments into a pBluescript KS(+) plasmid containing a cDNA clone of fungal ATP sulfurylase in which the wild type C-terminal 221 base pairs had been removed. All cloned PCR fragments were sequenced to ensure that the desired mutations were introduced. Sequenced ATP sulfurylase genes were cloned as NdeI-BglII fragments into the Novagen pET23a(+) plasmid and introduced into E. coli strain BL21(DE3) for protein expression.

Protein Expression and Purification. About 0.2 ml of an 8-hour culture was used to inoculate two 3-liter Fernbach flasks each containing 1000 ml of LB Amp medium. The cultures were grown aerobically at 37 C for 8-10 hours and then transferred to 15 C. Upon transfer to 15 C, 1 g of α-lactose was added per liter of culture to induce protein expression. After 8 - 10 hours at 15 C, the cells were harvested by centrifugation at 12000 x g for 10 minutes. Approximately 4-8 ml of packed cells were obtained. The cells were then resuspended in about 50 ml of chilled 40 mM Tris - Cl, pH 8.0 and lysed in a single pass through a Watts Fluidair Microfluidizer (model B12-04DJC M3). All subsequent steps were carried out at 4 C. Cell debris and unbroken cells were removed by centrifuging at 16000 x g for 10 minutes. The supernatant fluid was applied to a Blue Dextran (19) column (2.5 x 10 cm) that had been equilibrated with 40 mM Tris - Cl, pH 8.0. The column was then washed with the same buffer at 6 ml/min until the effluent had a A280nm of 0.005 or less. Protein was eluted with a linear gradient of NaCl (0-0.7

M) in 40 mM Tris-Cl, pH 8.0 (total volume 500 ml) at a flow rate of 2 ml per min. Seven-ml fractions were collected and their A280nm and ATP sulfurylase activity were

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measured. Fractions containing enzyme activity (coincident with the major protein peak) were pooled (total volume ca. 85 ml), dialyzed against 40 mM Tris - Cl, pH 8.0, and then applied to a DEAE-cellulose column (2.5 x 10 cm) equilibrated in the same buffer. After a brief wash, protein was eluted at 1 ml per min with a linear gradient of NaCl (0-0.4 M) in 40 mM Tris-Cl, pH 8.0 (total volume, 400 ml). Seven fractions containing ATP sulfurylase activity (total volume 49 ml) were pooled, divided into 1-ml aliquots, and stored frozen. A typical preparation yielded about 25 mg of pure enzyme. The A280nm/A260nm ratio of the enzymes ranged from 1.91 (for C509Y) to 2.01 (for

C509S). SDS gel electrophoresis indicated that all the enzymes were at least 95% pure. The absence of Cys-509 in the mutant enzymes was confirmed by demonstrating their lack of reactivity with DTNB in the absence of SDS (1). Chemicals and Coupling Enzymes. Most biochemicals, buffers, column media, and coupling enzymes were obtained from Sigma. PAPS was prepared as described previously (20). Concentrations of stock solutions were established by enzymatic analysis using Nuclease P1 coupled to ATP sulfurylase, hexokinase, and glucose-6-phosphate dehydrogenase in the presence of excess PPi, MgCl2, NADP+, and 1 mM

glucose. Protein Assays. ATP sulfurylase concentrations were determined from the relationship: concmg x ml-1 = A280nm/0.871 (21). (In theory, this results in a 3% error in

the assumed concentration of C509Y.) Enzyme Assays. ATP sulfurylase activity was characterized by the continuous, coupled spectrophotometric molybdolysis assay (22) in the presence of NADH, PEP, KCl, excess adenylate kinase, inorganic pyrophosphatase, sulfate-free pyruvate kinase + lactate dehydrogenase, and ca. 0.5 µg (0.02 units) of pure P. chrysogenum APS kinase (10, 22, 23) . The stoichiometry of the assay is 2 moles of NADH oxidized per mole of AMP formed. In addition to providing good sensitivity, this assay has the advantage in that both primary substrates, MgATP and MoO42---, are continuously regenerated. The APS

kinase serves to remove traces of APS formed from contaminating inorganic sulfate during the preincubation period (20). (APS is a potent product inhibitor of the enzyme whereas the small increment of PAPS formed is innocuous.) Unless indicated otherwise, all assays were conducted at 30 C, in 50 mM Tris-Cl, pH 8.0. The total MgCl2 present

was always 5 mM greater than that of the total ATP. The specific activities of the wild-type, C509S, and C509Y forms of the enzyme freshly purified from the E. coli expression

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system and assayed at 5 mM total ATP, 10 mM total Mg2+ (as MgCl2), and 10 mM MoO42--- were, in order, 20, 17, and 14.5 units x mg protein---1. One unit is the amount of

enzyme that catalyzes the formation of 1 µmole of primary product in one minute. Data Analysis. For each experimental velocity curve, the Vmax value and the Hill coefficient, nH, were determined by fitting the plotted v versus [substrate] data to the

Hill equation:

v = Vmax[S]nH

′ K + [S]nH [1]

Hill coefficients were also determined as the slope of the Hill plot --

logv

Vmax − v= n H log[S]− log ′ K

[2] -- in the region corresponding to 50% saturation (i.e., where log [v/(Vmax - v)] = 0) or

over the range corresponding to 10% - 90% saturation (14). Curve-fits were obtained using DeltaGraph 4.05c (Macintosh) with all points weighted equally. The nH of a single plot determined by the three methods generally agreed to within 0.1. The nH of

replicate curves obtained at different times generally agreed to within <0.15. While the Hill coefficient is useful for comparing the sigmoidicity of different velocity curves, ultimately, differences in nH need to be related to the complete velocity equation for an

allosteric bireactant enzyme (Appendix).

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RESULTS AND CONCLUSIONS

Kinetic Properties of Cys-509-Tyr. Fig. 1 shows the velocity curves of the C509Y mutant enzyme under standard assay conditions. The most striking feature of the curves is that they are sigmoidal in the absence of PAPS. In fact, the increase in nH with

increasing concentrations of the fixed cosubstrate is the same trend displayed by the wild-type enzyme after covalent modification of Cys-509 (data not shown)4. Up to this point, the results suggested that cooperative behavior is induced by either (a) increasing the bulk of the side chain at position 509 or (b) eliminating the negative charge (R-S---) at this position. It was thought that replacing Cys-509 with the slightly smaller and uncharged Ser might help to distinguish between these two possibilities. Kinetic Properties of Cys-509-Ser. Fig. 2 shows the velocity curves of the C509S enzyme at several different fixed concentrations of cosubstrate. In spite of the size similarity of Ser and Cys, the plots are again sigmoidal although compared to C509Y, C509S has a lower [S]0.5 for either substrate at any given concentration of cosubstrate. Also, unlike the curves shown in Fig. 1, the nH values of the v versus [MgATP] plots for

C509S do not change significantly with increasing [MoO42---]. At subsaturating MgATP, the v versus [MoO42---] curves are also sigmoidal, but nH approaches unity as the

concentration of MgATP approaches saturation. This trend is consistent with the preferential binding of MgATP to free E of the R state. That is, as the fixed [MgATP] approaches saturation, the enzyme is driven far toward the R state which binds MoO42---

in a normal hyperbolic manner. At 5 mM MgATP, the Km for MoO42--- is 0.1 mM, which

is the same as that of the noncooperative wild type enzyme. In terms of equation 9 (Appendix), Lapp for C509S at saturating MgATP (equivalent to Lc6) must be very small, implying that c is less than unity. The sigmoidicity of the v versus MoO42- plot at

sub-saturating MgATP can be attributed, at least in part, to the synergism between MgATP and MoO42---. That is, even if KibT = KibR (e = 1), and KmbT = KmbR (j = 1), the v

versus [B] plots can be sigmoidal at subsaturating [A] if (a) substrate A binds preferentially to the R state (c < 1), and (b) the substrates bind to the R state synergistically (f < 1). The last condition seems highly likely given that the R state should closely resemble the noncooperative wild type enzyme where the Km value for each substrate is smaller than the corresponding Ki value (1).

The bireactant kinetics of C509S are similar to those of the wild-type enzyme in the presence of PAPS5. Comparing the above results with those of the C509Y enzyme leads to the conclusions that either (a) substituting a Tyr residue for Cys-509 drives the

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enzyme much further toward the T state than does substituting a Ser at this position or (b) the T state induced by substituting Tyr at position 509 is structurally different from that induced by substituting Ser (see Discussion). In either case, the results show that cooperative behavior is a not simply a result of increasing the bulk of the residue at position 509. Either the negative charge on the side chain of Cys-509 plays a critical role in stabilizing the R state, or the side chain size is extremely important and any change will favor a shift to the T state.

Effect of a competitive inhibitor. Activation by a competitive inhibitor at low6

competitive substrate concentrations is a hallmark of true cooperative binding. As shown in Fig. 3, inorganic thiosulfate, an inhibitor competitive with SO42--- or MoO42---

(24), does exactly that. Activation by S2O32---

is also seen with the wild-type enzyme after

chemical modification of Cys-509 (2), or in the presence of PAPS (4, 20). Note that the experimental level of the not-competitive cosubstrate (MgATP) influences the effect of the competitive inhibitor. That is, the activation is eliminated by an MgATP concentration that is too low in the case of C509Y, or too high in the case of C509S. These opposite effects are consistent with the different effects of MgATP binding on the cooperativity of the two mutant enzymes as illustrated in Figures 1b and 2b. Kinetics at lower pH. The side chain of a Ser residue is not much smaller than that of a Cys residue, but unlike Ser, a substantial fraction of the Cys side chain may be ionized at the standard assay pH of 8.0. The observation that C509S is intrinsically cooperative raised the possibility that the charge on residue 509 plays a major role in stabilizing the R state. If the side chain of Cys-509 behaves normally (i.e., has a pKa of 8.0 - 8.5),

decreasing the assay pH from 8.0 to (e.g.) 6.5 would decrease the fraction of the residue in the Cys-S--- form significantly. It was of interest then to determine whether protonating the Cys anion of the wild type enzyme had the same effect as substituting Ser for Cys. As shown in Table I, decreasing the pH did indeed induce sigmoidal v versus [MoO42---] curves. Lowering the pH also decreased Vmax,app and increased the [S]0.5. But the wild type enzyme at pH 6.5 did not mimic C509S: First, the velocity curve remained sigmoidal at 5 mM MgATP (nH = 2.1). Second, the enzyme at pH 6.5 was activated by S2O32--- only at high concentrations of MgATP (data not shown). In these respects, the enzyme behaved like C509Y rather than C509S. Surprisingly, the nH of C509S also increased as the assay pH was decreased. (nH was 1.8 at pH 8.0 and 2.3 at

pH 6.5). Consequently, we can not conclude that the sigmoidicity induced in the wild

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type enzyme was solely a response to protonating Cys-509. Considering the pH range studied, it is likely that protonating one or more His residues can contribute to an R-T transition. Several His residues are located in the C-terminal domain, including one adjacent to Cys-509 (His-508). His has been shown to be essential for ATP sulfurylase activity (5, 9, 25, 26), a role that may account in part for the decrease in Vmax,app as the

pH was decreased. (A decrease in the fraction of the total ATP in the MgATP form may also have contributed to the decrease in Vmax, app and increase in [S]0.5 as the pH was

decreased.) The experiments described in Table I were conducted in MES-Tris buffers in which the MES concentration increased as the pH was decreased. However, MES per se was not responsible for the sigmoidicity as evidenced by the hyperbolic velocity curves obtained in 0.05M MES (plus Tris to pH 8). Effect of PAPS on C509S. It was of interest to determine whether PAPS had an additional effect on a mutant enzyme, or whether the mutation transformed the enzyme completely to the T state. As shown in Fig. 4, the nH value of C509S increased further as the concentration of PAPS was increased. At 240 µM [PAPS], the nH of the v versus

[MgATP] plot was nearly 3. Thus the Cys to Ser mutation promoted only a partial shift toward the T state allowing the R-T equilibrium to be driven further toward the T state or back toward the R state by the appropriate ligand. In this respect, C509S resembles a typical allosteric enzyme. The apparent nH limit of 3 (instead of 6) is very likely a

consequence of the nonexclusive binding of PAPS and/or substrates. However, the possibility that the enzyme behaves in an alternating ‘‘half-of-the-sites” manner can not be immediately discarded. The effect of PAPS on Vmax,app indicates that either (a) the

catalytic activity of the T state is much less than that of the R state, or (b) substrate binding to the T state is not highly synergistic, or (c) both conditions apply. In contrast to the results shown in Fig. 4, PAPS decreased the sigmoidicity of the v versus [MgATP] plot of C509Y: At 1 mM MoO42--- in the absence of PAPS, nH and Vmax,app were, respectively, 2.3 and 12.2 units x mg protein-1. At 240 µM PAPS, nH was 2.0; Vmax,app

decreased to 6.8 units x mg protein-1 (data not shown). Susceptibility of the C-Terminal domain to proteolysis. As shown in Fig. 5, treatment of wild type P. chrysogenum ATP sulfurylase with a low concentration of trypsin results in an initial rapid cleavage producing a well-defined product. Sequence analysis of the products revealed that the primary site of cleavage was at Lys-527, a residue that lies in a region analogous to the PAPS motif-containing mobile loop of true APS kinase and

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close to the analogous ‘‘quick trypsin’’ site of that enzyme (which is Arg-158) (11). In some incubations, cleavage at a second ‘‘quick trypsin’’ site of ATP sulfurylase (Arg-488) could be detected before the pattern was obscured by further proteolysis. MgATP, APS, or PAPS protected the wild type and C509S against proteolysis. C509Y was not protected. The pattern for the wild type enzyme in the presence of PAPS is shown in the second row of Fig. 5. Both mutant enzymes were cleaved much more rapidly than the wild type enzyme suggesting that the mobile loop/PAPS motif region is more accessible in the T state than in the R state. (The pattern for C509S is shown in the third row of Fig. 5.) Considering the sequence homology of the two enzymes and the similar locations of the primary ‘‘quick trypsin’’ sites (Fig. 6), it is likely that true APS kinase and the C-terminal domain of ATP sulfurylase have similar structures.

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DISCUSSION

Data obtained in the present study indicate that Cys-509 participates in stabilizing fungal ATP sulfurylase in an R state which binds both substrates hyperbolically with high affinity. The requirement for Cys at position 509 is quite strict. Replacing Cys-509 with tyrosine promotes the transition to a low-affinity T state. As a result, the v versus [MgATP] and v versus [MoO42---] curves are sigmoidal (in the absence of PAPS) with Hill coefficients, nH, that increase as the concentration of the

fixed substrate is increased. In this respect, C509Y behaves like the wild type enzyme covalently modified at Cys-509 by (e.g.,) DTNB, NEM, or tetrathionate. Substituting serine at position 509 also destabilizes the R state and again the result is sigmoidal velocity curves. The v versus [MgATP] curve remains sigmoidal at saturating MoO42- but the v versus [MoO42-] curve becomes hyperbolic at saturating MgATP7. These

kinetics indicate that MgATP has a higher affinity for the free E form of the R state compared to its affinity for free E of the T state, but that cosubstrate MoO42--- binds

more-or-less equally well to free E of both states. Stated alternatively, MgATP alone can trigger the T to R transition of C509S. The kinetic effects of substituting Ser at position 509 are the same as those promoted by the reversible binding of PAPS to the wild type enzyme. At first glance, there appears to be two different classes of kinetic response to alterations at position 509. The simplest explanation for the different kinetics is that there is a single T state, but different alterations in the region of Cys-509 cause a different extent of R to T transition, i.e., result in different base level values of the allosteric constant, L (13). The consequence of the difference is best appreciated by examining a plot of nH versus log L. If the T state has catalytic activity (even very low

compared to the R state), the plot is bell-shaped with limits of 1.0 (14, 27) . The effect of increasing the concentration of a ligand on nH depends on which side of the maximum

the enzyme is poised in the absence of ligands, i.e., whether the base level L is larger or smaller than the L at the maximum nH. Thus a decrease in the apparent L value (as

would occur when the fixed concentration of a cooperatively-bound cosubstrate is increased) could result in an increase or a decrease in nH. Whatever the effect of the fixed substrate concentration on nH, an increase in the apparent L (as would occur

when the concentration of the allosteric inhibitor is increased) will have the opposite effect. If this explanation is applicable, the different [S]0.5 values of the two mutant enzymes and the effects of changing [MgATP] or [PAPS] on nH mean that covalently

modifying or protonating the wild type enzyme, or replacing Cys-509 with Tyr drives

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the enzyme further toward the T state than does PAPS binding or replacement of Cys-509 with Ser. Another possible cause of the two classes of kinetics is that there are two types of T states. One type is produced by substituting Tyr for Cys at position 509, or by covalently modifying Cys-509 of the wild type enzyme, or by decreasing the pH below 8. The second type is formed when Cys-509 is replaced by Ser or when the wild type enzyme binds PAPS. In this scenario, the T to R transition of C509Y would be driven mainly by the formation of the R state ternary E.MgATP.MoO42- complex.

Compared to the wild type enzyme, the mutant enzymes have lower specific activities at saturating MgATP and MoO42--- (wild type > C509S > C509Y). If the VmaxR

values of the mutant enzymes are the same as that of the wild type enzyme, then their lower specific activities can be attributed to different base level L values, nonexclusive substrate binding, and a low activity T state (see Appendix, equation 12. For example, the molybdolysis Vmax of C509S (17 units x mg protein-1) is about 85% that of the wild

type enzyme suggesting that at saturating substrate levels, about 15% of the enzyme remains trapped in the very low activity T state. The dramatic change in kinetic properties resulting from the substitution of Tyr or Ser for Cys-509 confirms the key role of this position in holding the enzyme in the R state. As shown in Fig. 6, the residue analogous to Cys-509 in true APS kinase is Ala-145, which is located just before a mobile loop (residues 149 - 169) containing a putative PAPS motif (12). This loop is believed to serve as a hinged element (‘‘ATP lid’’) that immobilizes and protects bound MgATP in APS kinase (11). Ala-145 (and by inference, Cys-509) is located within a short helix at the N-terminal end of the loop. Although the C-terminal domain of ATP sulfurylase probably does not bind MgATP (because of alterations to the P-loop -- see (10)), a similar motion of the analogous mobile element may play a role in the R-T transition -- a suggestion consistent with the observations that (a) the primary ‘‘quick trypsin’’ site resides within the PAPS motif of the mobile loop and (b) that site is more accessible in the mutant enzymes (which exist primarily in the T state) than in the wild type enzyme (which exists almost entirely in the R state). If a movement of the loop does occur as part of the allosteric transition, one can understand why covalent modification or amino acid substitution within the small helix (hinge?) might alter the allosteric equilibrium. The facile dissociation and reassociation of subunits is another physical characteristic of APS kinase (28) that may have been recruited by ATP sulfurylase as part of the allosteric transition. Indeed, preliminary x-ray diffraction studies suggest that the R state of P. chrysogenum ATP sulfurylase has a

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trimer-of-dimers structure which is partially stabilized by interactions of C-terminal domains.

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APPENDIX: KINETIC BEHAVIOR OF A BIREACTANT COOPERATIVE ENZYME

The principles of the concerted transition (symmetry) model for cooperative enzymes (13, 27) can be extended to multireactant enzymes provided that rapid equilibrium conditions prevail (or are assumed) for the substrate binding steps and the allosteric transition (29). Compared to unireactant systems, the requirement that both substrates bind to the enzyme before any catalytic activity occurs adds an additional layer of complexity. For example, one or both of the substrates might bind cooperatively to the free enzyme, but neither substrate might bind cooperatively to the binary enzyme.cosubstrate complex. Conversely, only one or both of the substrates might bind cooperatively to the enzyme.cosubstrate complex, but neither might bind cooperatively to the free enzyme. Also, the binding of one substrate at the catalytic site may promote or may hinder the binding of the other substrate. This heterotrophic interaction can also affect the properties of the velocity curves. Because of these possibilities, the Hill coefficient for the varied substrate might increase, decrease, or remain the same as the concentration of the non-varied substrate is increased. The velocity equation for bireactant ATP sulfurylase in the presence of substrates A (MgATP) and B (MoO42---) which add in a rapid equilibrium random fashion is

shown below. The equation takes into account that X (PAPS), the allosteric effector, binds to the catalytic site as an inhibitor competitive with both MgATP and MoO42---, as

well as to the allosteric site (20).

v =num1 + num2

denom1 + denom2

[3] where:

num1 = VmaxTL 1+ [X]

KXT

n[A][B]

KiaT KmbT1 + [A]

KiaT+ [B]

KibT+ [A][B]

KiaTKmbT+ [X]

KixT

(n−1)

[4]

num2 = VmaxR

1+[X]KXR

n[A][B]

KiaRKmbR

1 +[A]KiaR

+[B]

KibR+

[A][B]KiaRKmbR

+[X]KixR

(n−1)

[5]

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denom1 = L 1+ [X]KXT

n

1+ [A]KiaT

+ [B]KibT

+ [A][B]KiaT KmbT

+ [X]KixT

n

[6]

denom2 = 1 + [X]KXR

n

1+ [A]KiaR

+ [B]KibR

+ [A][B]KiaR KmbR

+ [X]KixR

n

[7] KiaR and KibR are, respectively, the A and B dissociation constants of the R state EA and EB complexes. KmbR is the B dissociation constant from the R state EAB complex. KixR is the PAPS dissociation constant of the R state catalytic site. Kma does not appear in the equation, but for each state, Kma equals KmbKia/Kib.

KiaT, KibT, KmbT, and KixT are the corresponding T state catalytic site constants. KXT and KXR are the PAPS dissociation constants of the T state and R state allosteric

sites, respectively. Exponent n is the number of subunits in the oligomer, each one bearing a catalytic and an allosteric site. (For ATP sulfurylase, n = 6.) L is the allosteric constant, i.e., the [T]0/[R]0 ratio in the absence of ligands. VmaxR and VmaxT are the maximal velocities of the R and T states, respectively. (VmaxR = nkcatR; VmaxT = nkcatT.) The num1 term accounts for product formation by all T state complexes containing bound A and B. Similarly, num2 accounts for product formation by R state complexes containing both A and B. The denom1 term represents the concentrations of all T state species relative to [R]0. The denom2 term represents the concentrations of all R state species relative to [R]0.

If ligand concentrations and the catalytic rate constants are normalized to their respective R state constants (a common practice in displaying equations for this model -- (13, 30) ), the velocity can be written as:

vVmax,R

=

gLcαeβh

(1 + mγ)n 1 + cα + eβ +cαeβ

h+ qδ

n−1

+ αβf

(1 + γ )n 1 + α + β + αβf

+ δ

n−1

L(1+ mγ )n 1+ cα + eβ +cαeβ

h+ qδ

n

+ (1+ γ )n 1+ α + β + αβf

+ δ

n

[8]

where: α =

[A]KiaR

, β =

[B]KibR

, γ =

[X]KxR

, δ =

[X]KixR

, c =

KiaR

KiaT, e =

KibR

KibT,

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f = KmaR

KiaR

= KmbR

KibR

, h = KmaT

KiaT

= KmbT

KibT

, m = KxR

KxT

, q = KixR

KixT

, and

g =VmaxT

VmaxR

The terms c, e, and m are, in order, the non-exclusive binding coefficients of substrates A and B and allosteric inhibitor, X. The interaction factor f describes the effect of the binding of one substrate on the dissociation constant of the other substrate at the catalytic R site. Thus, if f < 1, the substrates bind synergistically. The factor h is the corresponding substrate interaction factor of the T state. Other coefficients that are sometimes useful for simplifying equations or describing kinetic properties are:

j = efh

= KmbR

KmbT

and p = KmaR

KmaT

When substrate A is saturating, the velocity at any [B] is given by:

v =gVmaxR

′ L cn [B]

KmbT

1+ [B]

KmbT

n−1

+ VmaxR

[B]

KmbR

1+ [B]

KmbR

n−1

′ L cn 1+ [B]

KmbT

n

+ 1+ [B]

KmbR

n

[9]

or:

v =

gVmaxR′ L cneβ

h1+ eβ

h

n−1

+ VmxR

βf

1+ βf

n−1

′ L cn 1 + eβh

n

+ 1+ βf

n

[10] where L’ is the apparent allosteric constant at the fixed [X] in the absence of other ligands:

′ L = L

1+ [X]

KXT

n

1+ [X]

KXR

n= L

(1+ mγ )n

(1+ γ )n

[11]

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KxT is expected to be < KxR (i.e., m >1). As X approaches saturation, L’ approaches a limit of L(KxR/KxT)n = Lmn.

The sigmoidicity of the v versus [B] plot at saturating A depends on several factors: (a) the nonexclusive binding coefficient for the interaction of B with the EA form of the T and R states, (KmbR/KmbT = j), (b) the magnitude of g, and most importantly,

(c) the magnitude of the apparent allosteric constant, which equals L’cn. It can be seen that if c is small (because substrate A binds preferentially to the free form of the R state), Lapp might be small even if L’ is substantial. In this case, the velocity curve at saturating

[A] will be hyperbolic (even though the plot may be sigmoidal at subsaturating [A]). It is possible to express c in terms of some other coefficients: c = ep/j = hp/f. The latter relationship reveals that Lapp at saturating [A] depends on the relative strengths of the

active site A/B interactions of the two states as well as on p. For example, if the binding of one substrate to the free E form of the R state increases the affinity for the other substrate (f < 1), and this synergism is greater than that which occurs at the T state active site, ( f < h), the cn factor could be a large number and consequently, Lapp could

be large yielding a sigmoidal velocity curve at saturating [A] even if L’ is not very large and p = 1. Similarly, if binding of one substrate to the free E form of the R state has no effect on the binding of the other (f = 1), but the binding of one substrate to the free E form of the T state hinders the binding of the other (h > 1), again f will be < h and a sigmoidal curve could result (30). If g • 1, the velocity given by equation [9] or [10] is a Vmax,app (for saturating A at a subsaturating level of B). But if g > 1 and KmbR < KmbT (i.e., the state with the

higher catalytic activity has the lower affinity for B), the v versus [B] curve might pass through a maximum and then decrease to a lower limit as [B] approaches saturation. The equation for v versus [A] at saturating B is symmetrical to that shown for saturating A. When both substrates are saturating, the limiting velocity in the absence of X is given by:

vlimit = VmaxR

(1+ gLapp )

(1 + Lapp ) = VmaxR

(1+ gLcn jn )

(1+ Lcn jn )

[12]

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If g = 1, the limiting velocity at saturating A and B will be independent of L’, c, and j, i.e., vlimit = VmaxR. But if the T state is less catalytically active than the R state (i.e., g <

1), vlimit can be < VmaxR.

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REFERENCES

1. Renosto, F., Schultz, T., Re, E., Mazer, J., Chandler, C. J., Barron, A., and Segel, I. H. (1985) J. Bacteriol. 164, 674 - 683. 2. Renosto, F., Martin, R. L., and Segel, I. H. (1987) J. Biol. Chem. 262, 16279 --- 16288. 3. Martin, R. L., Daley, L. A., Lovric, Z., Wailes, L. M., Renosto, F., and Segel, I. H. (1989) J. Biol. Chem. 264, 11768 - 11775. 4. Renosto, F., Martin, R. L., Wailes, L. M., Daley, L. A., and Segel, I. H. (1990) J. Biol. Chem. 265, 10300 - 10308. 5. Yu, M., Martin, R. L., Jain, S., Chen, L. J., and Segel, I. H. (1989) Arch. Biochem.

Biophys. 269, 156 - 174. 6. Renosto, F., Patel, H. C., Martin, R. L., Thomassian, C., Zimmerman, G., and Segel, I. H. (1993) Arch. Biochem. Biophys. 307, 272 - 285. 7. Osslund, T., Chandler, C., and Segel, I. H. (1982) Plant Physiol. 70, 39 - 45. 8. Renosto, F., Martin, R. L., Borrell, J. L., Nelson, D. C., and Segel, I. H. (1991) Arch. Biochem. Biophys. 290, 66 - 78. 9. Foster, B. A., Thomas, S. M., Mahr, J. A., Renosto, F., Patel, H., and Segel, I. H. (1994) J. Biol. Chem. 269, 19777 - 19786. 10. MacRae, I., Rose, A. B., and Segel, I. H. (1998) J. Biol. Chem. 273, 28583 - 28589. 11. MacRae, I. J., Segel, I. H., and Fisher, A. J. (2000) Biochemistry . 39, 1613 --- 1621. 12. Satishchandran, C., Hickman, Y. N., and Markham, G. D. (1992) Biochemistry 31, 11684 -11688. 13. Monod, J., Wyman, J., and Changeux, J.-P. (1965) J. Molec. Biol. 12, 88 - 118.

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14. Segel, I. H., (1993) Enzyme Kinetics: Behavior and Analysis of Rapid Equilibrium

and Steady-State Enzyme Systems. Wiley-Interscience, New York. 15. Ballio, A., Chain, E. B., Dentice di Accadia, F., Navizio, F., Rossi, C., and Ventura, M. T. (1959) Sel. Sci. Papers Istituto Superiore Sanita 2, 343 - 353. 16. Itahashi, M. (1961) J. Biochem. (Tokyo) 50, 52 - 61. 17. Renosto, F. and Segel, I. H. (1977) Arch. Biochem. Biophys. 180, 416 - 428. 18. Hanson, A. D., Rathinasabapathi, B., Chamberlin, B., and Gage, D. A. (1991) Plant Physiol. 97, 1199 - 1205. 19. Ryan, L. D. and Vestling, C. S. (1974) Arch. Biochem. Biophys. 160, 279 - 284. 20. MacRae, I. and Segel, I. H. (1997) Arch. Biochem. Biophys. 337, 17 - 26. 21. Tweedie, J. W. and Segel, I. H. (1971) Prep. Biochem. 1, 91 - 117. 22. Segel, I. H., Renosto, F., and Seubert, P. A., in Methods in Enzymology Jakoby, W. B. and Griffith, O. W., Eds. (Academic Press, San Diego, 1987), vol. 143: Sulfur and Sulfur Amino Acids, pp. 334 - 349. 23. Renosto, F., Seubert, P. A., and Segel, I. H. (1984) J. Biol. Chem. 259, 2113 --- 2123. 24. Seubert, P. A., Hoang, L., Renosto, F., and Segel, I. H. (1983) Arch. Biochem.

Biophys. 225, 679 - 691. 25. Venkatachalam, K. V., Fuda, H., Koonin, E. V., and Strott, C. A. (1999) J. Biol.

Chem. 274, 2601 - 2604. 26. Deyrup, A. T., Singh, B., Krishnan, S., Lyle, S., and Schwartz, N. B. (1999) J. Biol.

Chem. 274, 28929 - 28936. 27. Rubin, M. M. and Changeux, J.-P. (1966) J. Mol. Biol. 21, 265 - 274.

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28. Renosto, F., Seubert, P. A., Knudson, P., and Segel, I. H. (1985) J. Biol. Chem. 260, 1535 - 1544. 29. Pettigrew, D. W. and Frieden, C. (1977) J. Biol. Chem. 252, 4546 - 4551. 30. Wood, H. G., Davis, J. J., and Lochmüller, H. (1966) J. Biol. Chem. 241, 5692 - 5704. 31. Storer, A. C. and Cornish-Bowden, A. (1976) Biochem. J. 159, 1 - 5.

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FOOTNOTES

*The research described in this paper was supported by NSF Grant MCB 9904003 to I. H. Segel. and A. J. Fisher. I. J. MacRae was supported in part by a Biochemistry and Molecular Biology Training Grant. E. Hanna and J. D. Ho were undergraduate honors research students. A preliminary report was presented at the 18

th International

Congress of Biochemistry and Molecular Biology, Birmingham, England, July, 2000. ¶Corresponding author. e-mail: ihsegel@ucdavis.edu; Tel.: 530-752-3193; Fax: 530-752-3085. 1 Abbreviations used: APS, adenosine 5’-phosphosulfate (adenylylsulfate); PAPS, 3’-phosphoadenosine 5’-phosphosulfate (3’-phosphoadenylylsulfate) MgATP, Magnesium chelate of ATP. ‘‘MgATP’’ solutions contained the indicated concentration of total ATP plus a 5 mM excess of MgCl2 thereby maintaining a constant fraction of the total ATP in

the MgATP form (ca. 90% at pH 8.0) as the nucleotide concentration was varied (30, 31) ; NEM, N-ethylmaleimide; DTNB, 5’, 5’ - dithiobis-(2-nitrobenzoate); MES, (2-[N-morpholino]ethanesulfonic acid; PCR, polymerase chain reaction; nH, Hill coefficient,

SDS, sodium dodecylsulfate; DTT, dithiothreitol. 2 Among fungal ATP sulfurylases that have been examined so far, two Cys residues (Cys-42 and Cys 509) are conserved. The third one in P. chrysogenum (Cys-68) replaces a Val that is present at that position in other fungal ATP sulfurylases. 3 For a while, the Genbank entry for P. chrysogenum ATP sulfurylase (A53651) described the enzyme as a ‘‘probable PAPS synthetase’’ and suggested that the enzyme possesses APS kinase activity. This information (which was not submitted by us) is incorrect and contrary to published accounts. The homogeneous enzyme does not have measurable APS kinase activity (< 0.001 units x mg protein-1 under standard assay conditions where true APS kinase from P. chrysogenum exhibits about 25 units x mg protein-1). Yeast ATP sulfurylase (Genbank S55198) was described in similar terms. But this enzyme is even less likely to possess APS kinase activity considering that it does not possess an APS kinase-like region. In contrast, the enzyme from Aquifex aeolicus (Genbank AE000722), which also possesses a C-terminal APS kinase - like domain, may very well be bifunctional considering the similarity of the P-loop and PAPS motif sequences to those of true APS kinases.

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4 The native enzyme modified with NEM at Cys-509 yielded the following data: The nH of the v versus [MgATP] plots of increased from 1.2 at 0.2 mM MoO42--- to 2.0 at 5 mM MoO42---. The nH of the v versus [MoO42---] plots increased from 1.8 at 0.3 mM MgATP to

2.1 at 5 mM MgATP. 5The wild type enzyme yielded the following data at 50 µM PAPS: The nH of the v versus [MgATP] plots varied from ca. 1.5 at 0.1 mM MoO42--- to 1.7 at 1 mM MoO42--- . The nH of the v versus [MoO42---] plots decreased from ca. 2 at 0.05 mM MgATP to ca. 1

at 2.5 mM MgATP. 6 Exactly how ‘‘low’’ the competitive substrate must be in order to demonstrate activation is best established by trial and error. For a simple unireactant system where

S and I bind exclusively to the R state, the peak velocity occurs at θ = L(n −1)n − α −1

where θ = [I]/Ki and α = [S]/Ks. Thus as the fixed [S] is increased, the peak moves

closer to the vertical axis and eventually disappears. 7 A number of years ago, Pettigrew and Frieden (30) warned that ‘‘the assumption that effects of the second substrate upon kinetic behavior may be ignored as long as it is at a saturating concentration may be invalid and lead to incorrect predictions...’’ The experimental effects of the non-varied substrate on cooperativity presented in this present report (Figs. 1 and 2) confirm that warning.

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LEGENDS TO FIGURES

Fig. 1. Velocity curves of C509Y. (a) v versus [MgATP] at pH 8.0 and the indicated fixed concentrations of molybdate. (b) v versus [MoO42---] at pH 8.0 and the indicated

fixed concentrations of MgATP.

Fig. 2. Velocity curves of C509S. (a) v versus [MgATP] at pH 8.0 and the indicated fixed concentrations of molybdate. Inset: Velocity curve at 7.5 mM MoO42---. (b) v versus [MoO42---] at pH 8.0 and the indicated fixed concentrations of MgATP. Inset: Velocity curve at 5 mM MgATP over a narrower MoO42--- concentration range. Curve fits of the 5 mM MgATP data to the Hill equation returned nH values of 1.04 to 1.05

(depending on the range covered). However, curve fits to the Henri-Michaelis-Menton equation (which fixes nH at 1.00) were, for all practical purposes, equally good (R2 in

both cases was > 0.999). Fig. 3. Activation of mutant enzymes by [S2O32---]. The enzymes were assayed at 0.1 mM MoO42--- and the indicated fixed concentrations of MgATP. Relative velocities, vi/v0, are plotted where vi is the velocity in the presence of S2O32- and v0 is the velocity

at the same substrate concentration in the absence of the inhibitor.

Fig. 4. Velocity curves of C509S at different [PAPS]. (a) v versus [MgATP] at 0.25 mM MoO42- and different fixed concentrations of PAPS. The nH of the curve at 240 µM

PAPS was obtained from a curve that extended to 10 mM MgATP. (b) v versus [MoO42---] at 0.1 mM MgATP and different fixed [PAPS].

Fig. 5. Proteolysis of P. chrysogenum ATP sulfurylase by trypsin. Each incubation mixture contained 0.3 mg of ATP sulfurylase and 0.7 µg of trypsin per ml in 50 mM Tris-Cl, pH 8.0. PAPS (when present) was 200 µM. Samples were withdrawn at the indicated times and added to an equal volume of boiling 40 mM Tris-Cl, pH 8.0 containing 5% SDS and 25 mM DTT. SDS electrophoresis was performed in a 12.5% homogeneous polyacrylamide gel. Each lane contained ca. 1.5 µg of protein. Gels were stained with Coomassie Blue. Fig. 6. Sequence comparison of true APS kinase and the C-terminal domain of ATP

sulfurylase from P. chrysogenum. The APS kinase sequence (Genbank U39393) has been corrected to show Gly instead of Arg at position 54. The ATP sulfurylase sequence

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26

(Genbank U07353) has been corrected to show a previously omitted Gly at position 369. Asterisks indicate the sites of rapid cleavage by trypsin. The black circles identify four of the hydrophobic residues that pack together at the dimer interface in APS kinase. The positions of the mobile loop in true APS kinase and of Cys-509 (“SH-1”) are also noted.

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TABLE I

Effect of pH on Some Kinetic Properties of Wild-Type P. chrysogenum ATP Sulfurylasea

pH nH [MoO42-

]0.5

Vmax,app

(mM) µmoles x min-1 x mg protein-1 8.0 1.06 0.32 17.2 7.5 1.16 0.42 16.3 7.0 1.66 0.48 14.2 6.5 2.30 0.72 12.8 aRates were measured at 0.25 mM MgATP as described in Material and Methods, except that the assay mixtures were buffered at the indicated pH value. The buffers were prepared by mixing 0.05 M MES, ‘‘free acid’’ with 0.05M Tris ‘‘free base’’ to the desired pH. Although the curve fit of the pH 8 data to the Hill equation yielded an nH of 1.06, the R2 value of the fit to the Henri-Michaelis-Menton equation (nH = 1.00) was

not significantly poorer. Lower pH values could not be studied because a protein precipitate would form in the assay mixtures.

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BB

B

B

B

B

B

B

B

B

B

B

B B BB

JJ

J

J

J

J

JJ

J

J

J

J

J

J

F F F F F F FF FF

FF F

F F

0

5

10

15

0 1 2 3 4 5 6

(a)

[MgATP] (mM)

[MoO42-]

10 mMnH = 2.3 Vmax = 13.8

nH = 2.0 Vmax = 8.3 0.5 mM

1.0 mMnH = 2.2 Vmax = 11.6

0.2 mM

nH = 1.6 Vmax = 1.9

nH = 1.7 Vmax = 4.00.3 mM

velo

city

(un

its x

mg

prot

ein-1

)Fig. 1a

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BBB

B

B

B

B

B

B

B

B

B

B

BB B B

HHHHH H

HH

H

H

JJJJ

JJ

J

J

J

J

JJ

J

J

J

J

0

5

10

15

0 2 4 6 8 10 12

nH = 2.2 Vmax = 14.0

(b)[MgATP]

5.0 mM

0.5 mM

0.25 mM

0.1 mM

[MoO42-] (mM)

0.15 mM

nH = 2.2 Vmax = 11.1

nH = 1.9 Vmax = 9.3

nH =1.6 Vmax = 5.5

nH = 1.5 Vmax = 2.2

velo

city

(un

its x

mg

prot

ein-1

)Fig. 1b

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FFFF

FF

F

F

F

F

F

F

F

F

F

F F

J

J

J

J

J

J

J

J

J

J

J

J J J

BBB

B

BB

B

B

B

B

BB

0

5

10

15

0 1 2 3[MgATP] (mM)

[MoO42-]

0.25 mM

0.5 mM

1.0 mMn

H= 1.8 Vmax 14.0

nH

= 1.8 Vmax = 10.7

nH

= 1.9 Vmax = 13.2

nH

= 1.9 Vmax = 9.0

0.15 mM

0.05 mMn

H= 1.9 Vmax = 5.5

v

[MgATP] mM

0

5

10

15

0 0.1 0.2

[MoO42-] = 7.5 mM

nH

= 1.8

Vmax

= 14.3

(a)

velo

city

(un

its x

mg

prot

ein-1

)Fig. 2a

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J

J

J

J

JJ

J

J

J

J

J

J

J

J

J

J

JJ J J

B

B

B

B

B

B

B

B

BB

B

B

B

0

2

4

6

8

10

12

14

16

18

0 1 2 3 4 5 6 7

[MgATP]

1 mM

0.1 mM

0.25 mM

0.05 mM

[MoO42-] (mM)

nH

= 1.8 Vmax = 9.9

nH

= 1.7 Vmax = 12

nH

= 1.7 Vmax = 13.9

nH

= 1.2 Vmax = 16.0

nH

= 1.0 Vmax = 16.6 5 mM

0

5

10

15

0 0.2 0.4 0.6 0.8[MoO4

2-]

v [MgATP] = 5 mM

(b)

nH = 1.0

velo

city

(un

its x

mg

prot

ein-1

)Fig. 2b

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BB

B

B

B

B

BB B

B

J

J

J

JJ J

J

J

JJ

J

H

HH

H

H

H

HHH

0.0

0.5

1.0

1.5

2.0

0 1 2 3

BBBBB

BB

B

B

B

B

B

JJJ J J

J

J

J

J

H

H

H

H

H

H

HH

HH H

0.0

0.5

1.0

1.5

0 2 4 6 8 10

[MgATP]

5 mM

1 mM

10 mM

C509Y

[S2O32-] (mM)

C509S

0.75 mM

5 mM

[MgATP]

(a)

(b)

[S2O32-] (mM)

0.25 mM

vi

v0

vi

v0

Fig. 3

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BBBBBB

B

B

B

B

B

B

B

BB B

F F FF

FFF

F

F

0

2

4

6

8

10

12

0 1 2 3 4[MgATP] (mM)

nH

= 1.9

Vmax

= 10.6

nH

= 2.4

Vmax

= 8.4

nH

= 2.9

Vmax

= 7.5

[PAPS]

0

80 µM

160 µM

240 µM

nH

= 2.9

Vmax

= 6.0

(a)ve

loci

ty (

units

x m

g pr

otei

n-1)

BB

B

BB

B

B

B

BB

B

B

BB

B

HHH

H

H

H

H

H

H

HH

H

H

HH

0

2

4

6

8

10

12

0 5 10 15 20

[PAPS]0

80 µM

160 µM

240 µMvelo

city

(uni

ts x

mg

prot

ein-1

)

nH

= 2.5

Vmax

= 3.7

nH

= 1.8

Vmax

= 11.8 nH

= 2.2

Vmax

= 11.3

nH

= 2.7

Vmax

= 7.0

[MoO42-] (mM)

(b)

Fig. 4

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wild-type

wild-type+PAPS

C509S

Incubationtime (min)

0 1 3.5 5 10 20 40 60

Fig. 5 by guest on A

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ownloaded from

APS KinaseATP Sulf

APS KinaseATP Sulf

APS KinaseATP Sulf

APS KinaseATP Sulf

APS KinaseATP Sulf

1

369

41

412

87

458

131

499

177

541

40

411

86

457

130

498

176

540

211

573

- - - - M S T N I T F H A S A - L T R - S E R T E L R N Q R G L T I W L T G L S A S G K S T- G A H I P E W F S Y P E V V K I L R E S N P P R A T - Q - G F T I F L T G Y M N S G K D A

L A V E L E H Q L V R D R G V H A Y R L D G D N I R F G L N K D L G F S K A D R N E N I R RI A R A L Q V T L N Q Q G G R S V S L L L G D T V R H E L S S E L G F T R E D R H T N I Q R

I A E V A K - L - F A D S N S I A I T S F I S P Y R K D R D T A R Q L H E V A T P G E E T GI A F V A T E L T R A G A A V I A A - - P I A P Y E E S R K F A R D A V S Q A - - G S F F -

L P F V E V Y V D V P V E V A E Q R D P K G L Y K K A R E G V I K E F T G I S A P Y E A P AL V H V A T - - - - P L E H C E Q S D K R G I Y A A A R R G E I K G F T G V D D P Y E T P E

N P E V H V K N Y E L P V Q D A V K Q I I D Y L D T K G Y L P A K K EK A D L V V D F - S K Q S V R S I V H E I I L V L E S Q G F L E R Q

*

*

*SH-1

396

539PAPS motif

Mobile loop in APS kinase

Fig. 6

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Ian J. MacRae, Eissa Hanna, Joseph D. Ho, Andrew J. Fisher and Irwin H. SegelC-Terminal Domain of P. chrysogenum ATP Sulfurylase

Induction of Positive Cooperativity by Amino Acid Replacements Within the

published online August 23, 2000J. Biol. Chem. 

  10.1074/jbc.M005992200Access the most updated version of this article at doi:

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