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Molecular Endocrinology, doi:10.1210/me.2005-0349
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Molecular Endocrinology 20 (4): 931-943
Copyright © 2006 by The Endocrine Society

Mechanisms of Ligand Binding to the Parathyroid Hormone (PTH)/PTH-Related Protein Receptor: Selectivity of a Modified PTH(1–15) Radioligand for G{alpha}S-Coupled Receptor Conformations

Thomas Dean, Agnes Linglart, Matthew J. Mahon, Murat Bastepe, Harald Jüppner, John T. Potts, Jr. and Thomas J. Gardella

Endocrine Unit (T.D., A.L., M.J.M., M.B., H.J., J.T.P., T.J.D.) and Department of Pediatrics (H.J.), Massachusetts General Hospital and Harvard Medical School, Boston, Massachusetts 02114

Address all correspondence and requests for reprints to: Thomas J. Gardella, Endocrine Unit, Massachusetts General Hospital, Boston, Massachusetts 02114. E-mail: gardella{at}helix.mgh.harvard.edu.


   ABSTRACT
TOP
 ABSTRACT
INTRODUCTION
 RESULTS
 DISCUSSION
 MATERIALS AND METHODS
 REFERENCES
 
Mechanisms of ligand binding to the PTH/PTHrP receptor (PTHR) were explored using PTH fragment analogs as radioligands in binding assays. In particular, the modified amino-terminal fragment analog, 125I-[Aib1,3,Nle8,Gln 10,homoarginine11,Ala12,Trp14,Tyr15]rPTH(1–15)NH2, 125I-[Aib1,3,M]PTH(1–15), was used as a radioligand that we hypothesized to bind solely to the juxtamembrane (J) portion of the PTHR containing the extracellular loops and transmembrane helices. We also employed 125I-PTH(1–34) as a radioligand that binds to both the amino-terminal extracellular (N) and J domains of the PTHR. Binding was examined in membranes derived from cells expressing either wild-type or mutant PTHRs. We found that the binding of 125I-[Aib1,3,M]PTH(1–15) to the wild-type PTHR was strongly (~90%) inhibited by guanosine 5'-O-(3-thio)triphosphate (GTP{gamma}S), whereas the binding of 125I-PTH(1–34) was only mildly (~25%) inhibited by GTP{gamma}S. Of these two radioligands, only 125I-[Aib1,3,M]PTH(1–15) bound to PTHR-delNt, which lacks most of the receptor’s N domain, and again this binding was strongly inhibited by GTP{gamma}S. Binding of 125I-[Aib1,3,M]PTH(1–15) to the constitutively active receptor, PTHR-H223R, was only mildly (~20%) inhibited by GTP{gamma}S, as was the binding of 125I-PTH(1–34). In membranes prepared from cells lacking G{alpha}S via knockout mutation of Gnas, no binding of 125I-[Aib1,3,M]PTH(1–15) was observed, but binding of 125I-[Aib1,3,M]PTH(1–15) was recovered by virally transducing the cells to heterologously express G{alpha}S. 125I-PTH(1–34) bound to the membranes with or without G{alpha}S. The overall findings confirm the hypothesis that 125I-[Aib1,3,M]PTH(1–15) binds solely to the J domain of the PTHR. They further show that this binding is strongly dependent on coupling of the receptor to G{alpha}S-containing heterotrimeric G proteins, whereas the binding of 125I-PTH(1–34) can occur in the absence of such coupling. Thus, 125I-[Aib1,3,M]PTH(1–15) appears to function as a selective probe of G{alpha}S-coupled, active-state PTHR conformations.


   INTRODUCTION
TOP
 ABSTRACT
 INTRODUCTION
RESULTS
 DISCUSSION
 MATERIALS AND METHODS
 REFERENCES
 
PTH AND PTHrP play critical roles in calcium homeostasis, tissue development, and bone remodeling. PTH and PTHrP use for these functions the PTH/PTHrP receptor (PTHR), a class 2 G protein-coupled receptor (GPCR). For both PTH and PTHrP, which in humans are polypeptides of 84 and 141 amino acids, respectively, the principal determinants of receptor-binding affinity map to the carboxy-terminal portion of the fully active (1–34) ligand fragment, whereas the principal determinants of receptor activation map to the amino-terminal portion of the ligand. Both PTH(1–34) and PTHrP(1–34) induce strong coupling of the PTHR to the adenylyl cyclase/cAMP pathway mediated by G{alpha}S but can also induce coupling to signaling pathways involving other G proteins, including G{alpha}q/11 (1, 2), G{alpha}i (3), and G{alpha}12/13 (4).

The mechanisms by which PTH(1–34) and PTHrP- (1–34) bind to the PTHR and induce receptor activation have been investigated through the complementary approaches of receptor mutagenesis/chimerization (5, 6, 7, 8) and photo-affinity cross-linking (9, 10, 11). The combined results of these studies have given rise to a bipartite model of ligand-receptor interaction. By this two-domain model, the carboxy-terminal portion of PTH(1–34) binds to the amino-terminal extracellular (N) domain of the receptor in an initial docking step, and then the amino-terminal portion of the ligand engages the extracellular loop/transmembrane domain, or juxtamembrane (J) region of the receptor to induce the conformational changes involved in receptor activation and G protein coupling (12, 13, 14). Accumulating data suggest that a similar two domain-binding mechanism may be used by other class 2 GPCRs, including the calcitonin receptor (15, 16), the secretin receptor (17, 18), the vasoactive intestinal peptide receptor (19), and the corticotropin-releasing factor receptor (20, 21, 22), each of which binds a peptide ligand approximately equal in length to PTH(1–34).

Although the amino-terminal portion of PTH contains the principal determinants of receptor activation, amino-terminal fragments of PTH, such as PTH(1–14), elicit only extremely weak (EC50 = 200 µM) cAMP responses in PTHR-expressing cells, and exhibit no binding activity in competition assays performed with 125I-PTH(1–34) radioligand (23). The weak activities of such amino-terminal PTH fragments, as compared with the nanomolar potencies of PTH(1–34) ligands, can largely be explained by the absence of the docking interactions that normally occur between the carboxy-terminal portion of PTH(1–34) and the N domain of the receptor, as postulated by the two-domain model outlined above. In a recent series of structure-activity relationship studies performed on the PTH(1–14) fragment, we identified a number of modifications that together enhance binding affinity and cAMP-stimulating potency of the fragment on the PTHR by as much as five orders of magnitude. One such analog resulting from this work, [Aib1,3,Gln10,Har11,Ala12,Trp14]PTH(1–14)NH2, is as potent as PTH(1–34) for stimulating cAMP formation in PTHR-expressing cells (24, 25, 26, 27). We have hypothesized that the modifications of these PTH(1–14) analogs improve binding interactions specifically to the J domain of the PTHR because the analogs exhibit the same potency on a PTHR derivative, PTHR-delNt, that lacks most of the receptor’s N domain, as they do on the intact PTHR. In contrast, unmodified PTH(1–34) is approximately 100-fold less potent on PTHR-delNt than it is on the intact PTHR (26, 27). In recent extensions of this work, we derived inactive congeners of the modified PTH(1–14) analogs, substituted at positions 1–3, that competitively inhibit the agonist action of not only modified PTH(1–14) analogs, but also that of unmodified PTH(1–34) (28), consistent with the evolving model of the PTH-PTHR binding and activation mechanism.

In further extensions of our PTH(1–14) analog work, we sought to develop an amino-terminal PTH analog that could be used as a PTHR radioligand for exploring the interactions that occur specifically between the amino-terminal pharmacophoric region of PTH and the juxtamembrane region of the receptor. We have thus developed [Aib1,3,Nle8,Gln10,Har11,Ala12,Trp14,Tyr15]PTH-(1–15)NH2, herein termed [Aib1,3,M]PTH(1–15), which, when radioiodinated on tyrosine15, binds effectively as a radioligand to both the intact PTHR and to PTHR-delNt, as shown in recent whole-cell binding assays (27, 28). Here, we use this PTH(1–15) analog radioligand, along with 125I-PTH(1–34), and, in some experiments, the antagonist radioligand, 125I-PTHrP(5–36) (28), to further analyze the ligand-binding mechanisms used by the PTHR. The results show that, in contrast to the binding of 125I-PTH(1–34), the binding of 125I-[Aib1,3,M]PTH(1–15) to the PTHR is strongly dependent on the G protein-coupling/activation status of the receptor.


   RESULTS
TOP
 ABSTRACT
 INTRODUCTION
 RESULTS
DISCUSSION
 MATERIALS AND METHODS
 REFERENCES
 
Binding Time Courses in HKRK-B7 Cell Membranes
We first examined the time courses of receptor association for the agonist radioligands 125I-PTH(1–34) and 125I-[Aib1,3,M]PTH(1–15), and that of the antagonist radioligand 125I-PTHrP(5–36) in membranes prepared from HKRK-B7 cells. These cells, derived from the porcine kidney cell line LLC-PK1, are stably transfected to express the human PTHR at a density of approximately 950,000 copies per cell (29). As shown in Fig. 1Go, 125I-PTH(1–34) reached a maximum level of binding by approximately 40 min (t1/2 = 12 min), 125I-[Aib1,3,M]PTH(1–15) reached a maximum level by approximately 90 min (t1/2 = 37 min) and 125I-PTHrP- (5–36) reached a maximum level within 5 min (t1/2 = 1.5 min). In these experiments, each radioligand was used at approximately the same concentration (~0.03 nM) and with the same concentration of PTHR (membrane protein = 20 ng/µl). The differences in the equilibration times observed for these radioligands thus may reflect, at least in part, differences in the mechanisms by which each radioligand binds to the PTHR.


Figure 1
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  		Fig. 1. Radioligand Association and Dissociation Time Courses in HKRK-B7 Cell Membranes

Panels A–C show the time courses of association of 125I-PTH(1–34) (A), 125I-[Aib1,3,M]PTH(1–15) (B) and 125I-PTHrP(5–36) (C) with the PTHR in HKRK-B7 cell membranes. The inset of panel C displays the early time point data for 125I-PTHrP(5–36) on an expanded time scale. Panels D–F show the dissociation of complexes formed by the same radioligands and HKRK-B7 cell membranes after a 90 min preincubation phase. The agonists, 125I-PTH(1–34) and 125I-[Aib1,3,M]PTH(1–15) were assessed in the absence (closed circles) and presence (open squares) of GTP{gamma}S (5 x 10–5 M, added at t = 0). Each graph shows aggregate data, expressed as a percent of the maximum, specifically bound radioactivity (SB), from four or more experiments. In Panels A–C, the total maximum binding (specific plus nonspecific) and nonspecific binding levels were 12,319 ± 1,518 cpm and 356 ± 52 cpm, respectively, for 125I-PTH(1–34) (total radioactivity was 23,631 ± 1,849 cpm, n = 5); 3,073 ± 505 cpm and 346 ± 85 cpm, respectively, for 125I-[Aib1,3,M]PTH(1–15) (total was 30,108 ± 1,674 cpm, n = 4) and 3,364 ± 233 cpm and 456 ± 60 cpm, respectively, for 125I-PTHrP (5–36) (total was 23,583 ± 1,899 cpm, n = 4). In Panels D–F, the total maximum binding at t = 0, and nonspecific binding were 13,347 ± 1,332 cpm and 1,203 ± 206 cpm, respectively, for 125I-PTH(1–34) (total radioactivity was 31,557 ± 2,178 cpm, n = 10); 3,012 ± 515 cpm and 647 ± 105 cpm, respectively, for 125I-[Aib1,3,M]PTH(1–15) (total was 38,522 ± 3,911 cpm, n = 7) and 4263 ± 811 cpm and 700 ± 110 cpm, respectively, for 125I-PTHrP(5–36) (total was 25,062 ± 1,610 cpm, n = 4). Values are means (±SEM). All reactions contained a membrane protein concentration of 20 ng/µl.

 
The time courses of dissociation of the complexes formed between each radioligand and the PTHR in HKRK-B7 cell membranes was then examined. A preincubation of radioligand and membranes of 90 min was used to allow for ligand·receptor complex formation, after which the dissociation phase was initiated by the addition of excess unlabeled peptide ligand. To gain information on the extent to which G protein interactions might modulate the stability of the complexes formed by the agonist radioligands, 125I-PTH(1–34) and 125I-[Aib1,3,M]PTH(1–15), the dissociation times of these complexes were assessed in the absence and presence of the nonhydrolyzable guanine nucleotide analog, guanosine 5'-O-(3-thio)triphosphate (GTP{gamma}S) (5 x 10–5 M). The data were fit to a biexponential decay equation so as to accommodate potential rapid (t1/2 ≤ 5 min) and slow components in the resulting curves. As shown in Fig. 1DGo, in the absence of GTP{gamma}S, only approximately 9% (time course parameter values provided were derived from the curve fits of the aggregate data shown in the figures) of the complexes formed with 125I-PTH(1–34) dissociated rapidly, whereas the remaining fraction dissociated slowly (t1/2 = ~180 min). The addition of GTP{gamma}S increased the fraction of 125I-PTH(1–34)·PTHR complexes that dissociated rapidly to 25%, whereas the remaining 75% of the complexes dissociated slowly (t1/2 = ~120 min). In the absence of GTP{gamma}S, the dissociation profile obtained with 125I-[Aib1,3,M]PTH(1–15) was similar to that obtained with 125I-PTH(1–34), in that 21% of the complexes dissociated rapidly and the remaining complexes dissociated slowly (t1/2 = ~230 min; Fig. 1EGo). Upon addition of GTP{gamma}S, however, most (86%) of the 125I-[Aib1,3,M]PTH(1–15)·PTHR complexes dissociated rapidly (Fig. 1EGo). With the antagonist, 125I-PTHrP(5–36), assessed only in the absence of GTP{gamma}S, nearly all (90%) of the complexes dissociated rapidly (Fig. 1FGo).

Equilibrium Binding in HKRK-B7 Cell Membranes
The above dissociation data suggested that the two agonist radioligands, 125I-PTH(1–34) and 125I-[Aib1,3,M]PTH(1–15) form complexes with the PTHR that have distinct sensitivities to GTP{gamma}S. We further explored this possibility by comparing the effects of GTP{gamma}S, at varying concentrations, on the binding levels attained by the two radioligands in reactions performed in HKRK-B7 cell membranes under approximate equilibrium conditions (90-min incubations). As shown in Fig. 2Go and Table 1Go, at the maximum concentration of 1 x 10–5 M, GTP{gamma}S only partially (22 ± 3%) inhibited the binding of 125I-PTH(1–34), whereas it nearly fully (88 ± 1%) inhibited the binding of 125I-[Aib1,3,M]PTH(1–15). These data are consistent with the above dissociation data because they confirm that the binding of 125I-[Aib1,3,M]PTH(1–15) to the PTHR is highly sensitive to GTP{gamma}S, whereas the binding of 125I-PTH(1–34) is not.


Figure 2
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  		Fig. 2. Effect of GTP{gamma}S on PTH Radioligand Binding to HKRK-B7 Cell Membranes

The effects of GTP{gamma}S on the binding of 125I-PTH(1–34) and 125I-[Aib1,3,M]PTH(1–15) to the PTHR in HKRK-B7 cell membranes were assessed in near-equilibrium reactions (90-min incubations). Shown are data (mean ± SEM) from six experiments, each performed in duplicate. Data are expressed as a percent of the total radioactivity specifically bound in the absence of GTP{gamma}S (SB). Values of total bound (specific plus nonspecific), nonspecifically bound (determined in wells containing 1 x 10–6 M unlabeled PTH(1–34) ligand), and total added radioactivity, were 6,487 ± 790 cpm, 2,387 ± 409 cpm, and 21,761 ± 1,394 cpm, respectively, for 125I-PTH(1–34) and 4,350 ± 521 cpm, 735 ± 147 cpm, and 34,123 ± 2,205 cpm, respectively, for 125I-[Aib1,3,M]PTH(1–15). Membrane protein concentrations were 10 ng/µl for 125I-PTH(1–34) and 100 ng/µl for 125I-[Aib1,3,M]PTH(1–15).

 

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  		Table 1. Competition Binding in HKRK-B7 Cell Membranes

 
We further compared the binding of PTH(1–34) and [Aib1,3,M]PTH(1–15) ligands to the PTHR by performing competition studies using 125I-PTH(1–34) and 125I-[Aib1,3,M]PTH(1–15) as tracer radioligands and varying concentrations of unlabeled PTH(1–34) and [Aib1,3,M]PTH(1–15) as competitors. As shown in Fig. 3AGo, unlabeled [Aib1,3,M]PTH(1–15) was 350-fold weaker than PTH(1–34) in inhibiting the binding of 125I-PTH(1–34) to the PTHR in HKRK-B7 cell membranes (IC50s = 284 ± 61 nM and 0.81 ± 0.08 nM, respectively, P = 0.0008, Table 1Go). In contrast, [Aib1,3,M]PTH(1–15) was as potent as PTH(1–34) in inhibiting the binding of 125I-[Aib1,3,M]PTH(1–15) tracer radioligand to these membranes (IC50s = 0.92 ± 0.17 nM and 0.82 ± 0.17 nM, respectively, P = 0.3; Fig. 3BGo and Table 1Go). The weak capacity of [Aib1,3,M]PTH(1–15) to inhibit the binding of 125I-[Aib1,3,M]PTH(1–34) to the PTHR is consistent with the hypothesis that the PTH(1–15) analog binds solely to the J domain of the PTHR, and that PTH(1–34) binds to both the N and J domains of the receptor, as outlined above, and examined further below.


Figure 3
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  		Fig. 3. Competition Binding in HKRK-B7 Cell Membranes

Competition binding experiments were performed using membranes prepared from HKRK-B7 cells, either 125I-PTH(1–34) (A) or 125I-[Aib1,3,M]PTH(1–15) (B) as tracer radioligands, and unlabeled PTH(1–34) (filled circles) or [Aib1,3,M]PTH(1–15) (open squares) as competitor ligands. Each graph shows data (means ± SEM) from nine experiments, each performed in duplicate. Data are expressed as a percent of the total radioactivity specifically bound (SB) in the absence of unlabeled ligand. In the experiments of panel A, the values of total binding (specific plus nonspecific), nonspecific binding, and total radioactivity added were 4,996 ± 628 cpm, 1,663 ± 271 cpm and 26,729 ± 1,995 cpm, respectively. In panel B, the corresponding values were 3,409 ± 416 cpm, 593 ± 108 cpm and 28,411 ± 2,625 cpm, respectively. Reactions contained a membrane protein concentration of 10 ng/µl (A) or 100 ng/µl (B).

 
Binding to an Amino-Terminally Truncated PTHR in COS-7 Cell Membranes
To analyze further the structural domains of the receptor involved in determining the binding affinity for PTH(1–34) and [Aib1,3,M]PTH(1–15), we used a PTHR construct, PTHR-delNt, that lacks most of the receptor’s N domain (27). In prior studies performed in intact COS-7 cells expressing PTHR-delNt, we found that 125I-[Aib1,3,M]PTH(1–15) bound nearly as well as it did to the wild-type PTHR, and, as expected, 125I-PTH(1–34) failed to bind (reflecting the importance of the N domain of the PTHR in initiating high-affinity binding of this ligand) (28) (and data not shown). In our initial experiments performed with membranes prepared from COS-7 cells transfected with PTHR-delNt, however, we observed little or no binding of 125I-[Aib1,3,M]PTH(1–15) (as well as no binding of 125I-PTH(1–34) radioligand). In an effort to increase binding of 125I-[Aib1,3,M]PTH(1–15) to PTHR-delNt in membranes, we cotransfected the cells with a mutant G{alpha}S protein, G{alpha}S({alpha}3/ß5) (30) that has been shown to increase the maximum binding capacity of the PTHR, as assessed with a 125I-PTHrP(1–36) radioligand analog (12). This effect of the mutant G{alpha}S is presumably due to its capacity to couple to the receptor, and to thus stabilize a high-affinity receptor state, more efficiently (without increasing basal signaling) than does wild-type G{alpha}S (30). This strategy indeed increased binding of 125I-[Aib1,3,M]PTH(1–15) to PTHR-delNt in COS-7 cell membranes and resulted in maximum binding levels that were approximately 3-fold above those observed in membranes prepared from mock-transfected COS-7 cells without, as expected, resulting in detectable 125I-PTH(1–34) binding].

In competition assays performed with these PTHR-delNt/G{alpha}S({alpha}3/ß5)-expressing membranes, the binding of 125I-[Aib1,3,M]PTH(1–15) was potently inhibited by unlabeled [Aib1,3,M]PTH(1–15) and only weakly inhibited by unlabeled PTH(1–34) (IC50s = 0.62 ± 0.08 nM and 350 ± 40 nM, respectively; P = 0.007, Fig. 4AGo and Table 2Go). These data, when considered together with the competition data obtained with the wild-type PTHR (Fig. 3Go), confirm the hypothesis that [Aib1,3,M]PTH(1–15) binds predominantly, if not exclusively, to the PTHR J domain. They also verify that unmodified PTH(1–34) depends strongly on interactions to the N domain of the receptor to achieve its high binding affinity for the intact PTHR.


Figure 4
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  		Fig. 4. Ligand Binding to an Amino-Terminally Truncated PTHR in COS-7 Cell Membranes

Membranes were prepared from COS-7 cells transiently cotransfected with the amino-terminally truncated PTHR, PTHR-delNt, and, to increase binding capacity, with G{alpha}S-{alpha}3ß5 (30 ), and used in competition binding (A) and time course dissociation assays (B). Panel A shows the capacity of unlabeled PTH(1–34) and [Aib1,3,M]PTH(1–15) to inhibit the binding of 125I-[Aib1,3,M]PTH(1–15) to the membranes. The data (means ± SEM) are from three representative experiments each performed in duplicate. A summary of these and all related competition data obtained in COS-7 cells is reported in Table 2Go. Data are expressed as a percent of the total radioactivity specifically bound (SB) in the absence of unlabeled ligand (B0). Panel B shows the time courses of dissociation of 125I-[Aib1,3,M]PTH(1–15)·PTHR-delNt complexes in the absence (filled circles) and presence of GTP{gamma}S (5 x 10–5 M, open squares). Data are expressed as a percent of the maximal specific binding observed at t = 0. Shown are aggregate data from nine experiments. In the experiments of panel A, values of total bound (specific plus nonspecific), nonspecifically bound and total added radioactivity were 2,421 ± 465 cpm, 460 ± 101 cpm and 21,311 ± 1,006 cpm, respectively. In panel B, the values of maximal total bound radioactivity at t = 0, nonspecific binding, and total radioactivity added were 2,602 ± 486 cpm; 166 ± 24 cpm, and 26,382 ± 2,456 cpm, respectively. Reactions contained a membrane protein concentration of 100 ng/µl.

 

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  		Table 2. Competition Binding in COS-7 Cell Membranes

 
We then assessed whether or not the absence of the receptor’s N domain affected the stability and GTP{gamma}S sensitivity of the complexes formed between the receptor (PTHR-delNt) and 125I-[Aib1,3,M]PTH(1–15). As shown in Fig. 4BGo, in the absence of GTP{gamma}S, 40% of the 125I-[Aib1,3,M]PTH(1–15)·PTHR-delNt complexes dissociated rapidly (t1/ 2 = ~1 min), and the remaining 60% dissociated slowly (t1/ 2 = ~300 min). The addition of GTP{gamma}S increased the fraction of rapidly dissociating complexes to 63%, and caused a modest increase in the dissociation rate for the remaining complexes (t1/2 = ~45 min). Removal of the receptor’s N domain therefore does not prevent the formation of stable complexes with the 125I-[Aib1,3,M]PTH(1–15) radioligand, nor the sensitivity of these complexes to GTP{gamma}S.

Binding to a Constitutively Active Mutant PTHR
The results so far suggested that 125I-[Aib1,3,M]PTH(1–15) binds selectively to a conformation of the PTHR J domain that is stabilized by the interaction of the receptor with a heterotrimeric G protein. Because heterotrimeric G proteins are thought to interact more efficiently with active-state receptor conformations than with inactive-state receptors (31), the results led us to further hypothesize that 125I-[Aib1,3,M]PTH(1–15) binds preferentially to an active-state PTHR conformation. To explore this, we used the constitutively active mutant PTHR, PTHR-H223R (32), which, like constitutively active GPCRs in general (31, 33), is thought to have a higher propensity to adopt an active-state conformation than does the wild-type receptor. We thus predicted that 125I-[Aib1,3,M]PTH(1–15) would bind to PTHR-H223R in a more stable, and less GTP{gamma}S-sensitive fashion than it does to the wild-type PTHR. Membranes were prepared from COS-7 cells transiently transfected with the wild-type PTHR or with PTHR-H223R and analyzed for binding 125I-PTH(1–34) and 125I-[Aib1,3,M]PTH(1–15). In homologous competition binding assays, PTHR-H223R exhibited the same apparent binding affinity for PTH(1–34) as did the wild-type PTHR (2.8 ± 1.1 nM and 3.5 ± 1.0 nM, respectively, P = 0.3; Table 2Go). Unexpectedly, PTHR-H223R exhibited an approximate 15-fold lower apparent affinity for [Aib1,3,M]PTH(1–15) than did the PTHR (2.0 ± 0.6 nM and 0.13 ± 0.02 nM, respectively, P = 0.03; Table 2Go). The reason for this lower apparent binding affinity for [Aib1,3,M]PTH(1–15) on PTHR-H223R is not clear at present. In any case, the maximum specific binding levels attained by both 125I-PTH(1–34) and 125I-[Aib1,3,M]PTH(1–15) radioligands on PTHR-H223R were sufficient to permit analysis of the effects of GTP{gamma}S on this binding and the stability of the resultant ligand-receptor complexes.

As shown in Fig. 5Go, the binding of each radioligand to PTHR-H223R was indeed less sensitive to GTP{gamma}S than was its binding to the wild-type PTHR. Thus, GTP{gamma}S maximally (1 x 10–4 M) inhibited the binding of 125I-PTH(1–34) to the wild-type PTHR by 33 ± 3% and to PTHR-H223R by 17 ± 3% (P = 0.0007; Fig. 5AGo). Likewise, GTP{gamma}S maximally inhibited the binding of 125I-[Aib1,3,M]PTH(1–15) to the wild-type PTHR by 85±2% and to PTHR-H223R by 21 ± 2% (P = < 0.0001; Fig. 5BGo). As with the wild-type PTHR, the binding of 125I-[Aib1,3,M]PTH(1–15) to PTHR-delNt was nearly fully (88 ± 1%) inhibited by GTP{gamma}S (Fig. 5BGo).


Figure 5
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  		Fig. 5. Capacity of GTP{gamma}S to Inhibit PTH Radioligand Binding to Wild-Type and Mutant PTHRs in COS-7 Cell Membranes

Shown are the effects of varying concentrations of GTP{gamma}S on the binding of 125I-PTH(1–34) (A) and 125I-[Aib1,3,M]PTH(1–15) (B) to membranes prepared from COS-7 cells transiently transfected with the wild-type PTHR (filled circles), the constitutively active mutant, PTHR-H223R (open squares) or PTHR-delNt (cotransfected with G{alpha}S-{alpha}3ß5; open triangles, panel B only). Data (means ± SEM) are from six experiments, each performed in duplicate, and are expressed as a percent of the total radioactivity specifically bound in the absence of GTP{gamma}S (SB). In panel A, the total amount of 125I-PTH(1–34) radioactivity bound (specific plus nonspecific) to the wild-type PTHR was 4,499 ± 828 cpm and that to PTHR-H223R was 4,361 ± 833 cpm; nonspecific binding was 574 ± 106 cpm and total radioactivity added was 23,651 ± 1,649 cpm. In panel B, the total amount of 125I-[Aib1,3,M]PTH(1–15) radioactivity bound to the wild-type PTHR was 3,994 ± 1,460 cpm, that to PTHR-H223R was 3,158 ± 1,063 cpm, and that to PTHR-delNt was 1,998 ± 264 cpm; nonspecific binding was 430 ± 51 cpm and total radioactivity added was 25,942 ± 2,185 cpm. Reactions contained a membrane protein concentration of 100 ng/µl.

 
In time course dissociation assays performed in the absence of GTP{gamma}S, the fraction of stable complexes (t1/2 > 5 min) formed by either radioligand with PTHR-H223R was approximately 30% higher than the corresponding fraction observed with the wild-type PTHR: 92% vs. 66% for 125I-PTH(1–34) (Fig. 6Go, A and B, filled symbols), and 84% vs. 51% for 125I-[Aib1,3,M]PTH(1–15) (Figs. 6Go, C and D, filled symbols). The addition of GTP{gamma}S caused little or no change in the fraction of stable complexes formed by either radioligand and PTHR-H223R (Fig. 6Go B and D), whereas it decreased the fraction of stable complexes formed by 125I-PTH(1–34) and the wild-type PTHR by approximately 10%, and those formed by 125I-[Aib1,3,M]PTH(1–15) and the wild-type PTHR by approximately 30% (Fig. 6Go, A and C). The overall data obtained with PTHR-H223R are thus consistent with the hypothesis that 125I-[Aib1,3,M]PTH(1–15) binds preferentially to active-state conformations of the PTHR (which can be stabilized by the activating receptor mutation, His223->Arg, and/or coupling of the receptor to a heterotrimeric G protein).


Figure 6
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  		Fig. 6. Dissociation of Radioligands from the Wild-Type PTHR and a Constitutively Active Mutant PTHR in COS Cell Membranes

Membranes were prepared from COS-7 cells transiently transfected with either the wild-type PTHR (PTHR-WT) (A and C) or with PTHR-H223R (B and D) and, after a 90-min ligand-receptor complex formation phase, the dissociation of complexes formed with either 125I-PTH(1–34) (A and B) or 125I-[Aib1,3,M]PTH(1–15) (C and D) was assessed either in the absence (filled circles) or presence of GTP{gamma}S (5 x 10–5 M final concentration, open squares, dashed lines). Shown are aggregate data, expressed as a percent of the maximal specific binding observed at t = 0 (SB), from six (A and B) or eight (C and D) experiments. Values of maximal total binding (specific plus nonspecific) at t = 0 for 125I-PTH(1–34) on the PTHR, and on PTHR-H223R, were 7,742 ± 1,867 cpm and 6,073 ± 787 cpm, respectively; the corresponding values for 125I-[Aib1,3,M]PTH(1–15) were 3,857 ± 688 cpm and 2,955 ± 471 cpm, respectively. Values of nonspecific binding and total radioactivity were 728 ± 182 cpm and 37,024 ± 10,423 cpm, respectively, for 125I-PTH(1–34), and 223 ± 44 cpm and 27,805 ± 1,744 cpm, respectively, for 125I-[Aib1,3,M]PTH(1–15). Reactions contained a membrane protein concentration of 100 ng/µl.

 
Binding to Membranes Lacking G{alpha}S
The adenylyl cyclase/cAMP pathway is generally considered to be the principal signaling cascade to mediate the biological actions of the PTHR in vivo. Our current binding data obtained using cell membrane preparations are largely consistent with such a linkage for [Aib1,3,M]PTH(1–15), in that they demonstrate GTP{gamma}S sensitivity. They also suggest, however, that G{alpha}S-containing G protein heterotrimers are not essential for high-affinity binding of PTH(1–34) because GTP{gamma}S insensitivity was observed for this radioligand. We thus sought to specifically investigate the role that this G{alpha}-subunit plays in modulating the receptor’s affinity for PTH ligands. To do this, we used membranes prepared from a line of mouse embryonic fibroblast cells (34) that lack functional G{alpha}S due to homozygous disruption of the Gnas gene. These cells do not express detectable levels of the PTHR (34) and so were infected with an adenovirus vector encoding the PTHR to augment receptor expression. Parallel sets of cells were infected either with or without a second adenovirus vector encoding G{alpha}S, to thus obtain G{alpha}S+ and G{alpha}S– cells, each expressing the PTHR. The binding of 125I-PTH(1–34) and 125I-[Aib1,3,M]PTH(1–15) to membranes prepared from these cells was then assessed over a range of membrane protein concentrations. Figure 7AGo shows that 125I-PTH(1–34) bound nearly as well to membranes derived from the G{alpha}S– cells as it did to those derived from the G{alpha}S+ cells. In contrast, Fig. 7BGo shows that 125I-[Aib1,3,M]PTH(1–15) bound only to membranes prepared from the G{alpha}S+ cells. These results demonstrate that G{alpha}S plays a major role in determining the PTHR’s capacity to bind 125I-[Aib1,3,M]PTH(1–15) but is not required for binding 125I-PTH(1–34).


Figure 7
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  		Fig. 7. Radioligand Binding to the PTHR in Membranes from G{alpha}S– Cells

Membranes were prepared from mouse embryonic fibroblast cells that lack G{alpha}S due to homozygous disruption of Gnas and heterologously express via adenovirus-mediated transduction either the PTHR alone (open circles) or the PTHR and functional G{alpha}S (filled circles), and then tested at varying membrane protein concentrations for the capacity to bind 125I-PTH(1–34) (A) or 125I-[Aib1,3,M]PTH(1–15) (B). Reaction incubations were performed for 90 min. The amount of specifically bound radioactivity observed (SB) for each radioligand is expressed as a percent of the total amount of radioactivity added to the well. Shown are data (means ± SEM) from seven experiments, each performed in duplicate. The mean values of total binding (specific plus nonspecific) at the highest concentration of protein tested for the membranes derived from the G{alpha}S– and G{alpha}S+ cells were 7,450 ± 1,166 cpm and 9,196 ± 1,003 cpm, respectively, for 125I-PTH(1–34), and 577 ± 105 cpm and 5,177 ± 491 cpm, respectively, for 125I-[Aib1,3,M]PTH(1–15). The corresponding values of nonspecific binding (averaged from reactions performed at each protein concentration in the presence of 1 x 10–6 M unlabeled ligand), and total radioactivity added were 1,155 ± 245 cpm and 27,343 ± 5,541 cpm, respectively, for 125I-PTH(1–34), and 347 ± 46 cpm and 44,777 ± 5,887 cpm for 125I-[Aib1,3,M]PTH(1–15).

 

   DISCUSSION
TOP
 ABSTRACT
 INTRODUCTION
 RESULTS
 DISCUSSION
MATERIALS AND METHODS
 REFERENCES
 
In this study, we employed structurally distinct PTH radioligand analogs and membranes prepared from cells expressing altered forms of the PTHR, or altered with respect to their G protein expression status, to further dissect the mechanisms of ligand binding to the PTHR. Our main findings were that: 1) 125I-PTH(1–34) and the modified amino-terminal agonist analog, 125I-[Aib1,3,M]PTH(1–15), dissociated from the PTHR with complex kinetics exhibiting rapid and slow components, whereas the antagonist, 125I-PTHrP(5–36), dissociated with primarily rapid kinetics; 2) GTP{gamma}S strongly destabilized 125I-[Aib1,3,M]PTH(1–15)·PTHR complexes but only mildly destabilized 125I-PTH(1–34)·PTHR complexes; 3) removal of the receptor’s amino-terminal domain strongly diminished the binding affinity of PTH(1–34) but only mildly affected the binding affinity of [Aib1,3,M]PTH(1–15); 4) both 125I-[Aib1,3,M]PTH(1–15) and 125I-PTH(1–34) formed more stable and less GTP{gamma}S-sensitive complexes with the constitutively active receptor, PTHR-H223R, than they did with the wild-type PTHR; and 5) for the wild-type PTHR, G{alpha}S was required for binding 125I-[Aib1,3,M]-PTH(1–15) but not for binding 125I-PTH(1–34). The data from these studies add to those acquired in prior binding studies performed on the PTHR using the membrane assay approach (12, 35, 36), as well as to those acquired in whole cells using the photo-affinity cross-linking (9, 10, 37) and receptor mutational approaches (7), which together have provided much of the groundwork for current models of the PTH/PTHR interaction mechanism (14). Many areas of uncertainty remain in understanding this mechanism, including the precise roles that the various domains of the ligand and receptor play in the formation, stability and conformational dynamics of the ligand-receptor complex, and the role that G protein coupling plays in the ligand-binding process, particularly in terms of its effects on interactions that occur to the N and J domains of the receptor. The present studies were designed to address some of these issues.

One unexpected observation made in our studies was the pronounced difference in GTP{gamma}S sensitivities of the binding of 125I-PTH(1–34) to the PTHR, vs. the binding of 125I-[Aib1,3,M]PTH(1–15). This difference suggests that the PTHR can form at least two types of receptor conformations that display high affinity for agonist ligands. One type, revealed by the binding analyses of PTH(1–34), apparently does not require coupling to a heterotrimeric G protein for the formation of stable complexes with PTH(1–34) ligands. Another type, revealed with 125I-[Aib1,3,M]PTH(1–15), is dependent on coupling to a G protein heterotrimer, specifically one containing G{alpha}S. We also found that the constitutively active PTHR, PTHR-H223R, binds both [Aib1,3,M]PTH(1–15) and PTH(1–34) in a GTP{gamma}S-insensitive fashion (Figs. 5Go and 6Go); this finding suggests yet another type of high-affinity receptor conformation that occurs in the presence of the His223->Arg mutation. These findings overall support the view that GPCRs in general (31, 38), and the PTHR in particular (39, 40, 41) can adopt at least several different conformations and thereby exhibit an ensemble of ligand-binding and/or signaling functionalities. In this regard, the slower equilibration times seen in our association time course studies for the agonists, 125I-PTH(1–34) and 125I-[Aib1,3,M]PTH(1–15), vs. the faster equilibration time seen for the antagonist 125I-PTHrP(5–36) (Fig. 1Go, A–C), could potentially reflect rate-limiting conformational changes involved in the binding of the agonists that are absent in the binding of the antagonist (42).

Our data also provide information on the structural domains of the ligand and receptor that are likely to play a role in the formation and/or stabilization of distinct conformational states of the PTHR. The data showing high-affinity, GTP{gamma}S-sensitive binding of [Aib1,3,M]PTH(1–15) to PTHR-delNt (Figs. 4Go, A and B, and 5BGo) indicate that neither the (16–34) portion of the ligand, nor the N-domain of the receptor is required for the formation of the high-affinity receptor conformation that is bound by 125I-[Aib1,3,M]PTH(1–15), nor for the stabilization of this conformation by G protein. Both the (16–34) portion of the ligand and the N domain of the receptor are, however, required for the formation/stabilization of the high-affinity receptor conformation that is bound by unmodified PTH(1–34) in the apparent absence of coupling to a G protein heterotrimer. This is shown by the failure of 125I-[Aib1,3,M]PTH(1–15) to form a stable complex with the PTHR in the presence of GTP{gamma}S (Fig. 1EGo), and by the failure of 125I-PTH(1–34) radioligand to bind detectably to PTHR-delNt. The importance of the PTHR N domain in determining the overall affinity with which PTH(1–34) binds to the PTHR is further shown by our competition studies performed in COS-7 cell membrane using 125I-[Aib1,3,M]PTH(1–15) as a radioligand. In these studies, the potency with which PTH(1–34) inhibited the binding of 125I-[Aib1,3,M]PTH(1–15) to PTHR-delNt was 4000-fold weaker than the potency with which it inhibited the binding of this radioligand to the intact PTHR (350 ± 40 nM vs. 0.091 ± 0.038 nM; P = 0.007; Table 2Go). Related to these observations, in binding studies performed with the intact PTHR in HKRK-B7 cell membranes, we observed that unlabeled [Aib1,3,M]PTH(1–15), at a concentration of 1 x 10–5 M, nearly fully inhibited the binding of 125I-PTH(1–34) radioligand (Fig. 3AGo). Given that [Aib1,3,M]PTH(1–15) occupies only the J domain binding site of the receptor, this finding suggests that interactions between 125I-PTH(1–34) and the PTHR N domain are not, by themselves, strong enough to enable high-affinity binding, or detection of simultaneous binding of 125I-PTH(1–34) and [Aib1,3,M]PTH(1–15) to the receptor, via binding to the N and J domain sites, respectively (12), at least under the reaction conditions used here.

One of the more interesting inferences that may be taken from this work is that 125I-[Aib1,3,M]PTH(1–15) is a selective probe of an active-state conformation of the PTHR J domain that is stabilized by coupling of the receptor to a heterotrimeric G protein, specifically one containing G{alpha}S. The data supporting this conclusion include the nearly complete disruption of both 125I-[Aib1,3,M]PTH(1–15)·PTHR and 125I-[Aib1,3,M]PTH(1–15)·PTHR-delNt complexes by GTP{gamma}S (Figs. 1EGo, 4BGo, and 5BGo); the GTP{gamma}S-insensitive binding of 125I-[Aib1,3,M]PTH(1–15) to the constitutively active receptor, PTHR-H223R (Figs. 5BGo and 6DGo); the failure of 125I-[Aib1,3,M]PTH(1–15) to bind to membranes prepared from cells lacking G{alpha}S (Fig. 7AGo), and the restoration of this binding upon reintroduction of functional G{alpha}S (Fig. 7BGo). In contrast to these findings with 125I-[Aib1,3,M]PTH(1–15), the data with 125I-PTH(1–34), showing that as much as 75% of the complexes formed with the wild-type PTHR are stable in the presence of GTP{gamma}S (Figs. 1DGo and 5AGo), suggest that this intact radioligand can bind to a distinct high-affinity receptor conformation. In line with this interpretation, the GTP{gamma}S treatments used in our experiments appeared to adequately saturate the G proteins in the membrane preparations because they resulted in nearly full inhibition of the binding of 125I-[Aib1,3,M]PTH(1–15). A GTP{gamma}S-insensitive high-affinity receptor conformation was recently described for the related corticotropin-releasing factor receptor, and termed in this study R0 (43). Stable agonist ligand·receptor complexes in the presence of GTP{gamma}S have also been observed for several other class 2 GPCRs, including the calcitonin gene-related peptide receptor (44), the calcitonin receptor (45) and the glucagon receptor (46), each of which couples to G{alpha}S and binds a peptide ligand similar in size to PTH(1–34). The molecular nature of this putative GTP{gamma}S-insensitive, high-affinity ligand-receptor state (R0) is unclear, but it is intriguing to consider the possibility that the capacity for its formation is a general property of the class 2 GPCRs, and that it might play some role in the biological activities of these receptors, for example, by enabling catalytic G protein activation (47, 48, 49), or modulating receptor down-regulation/desensitization responses (45, 49). Such capacity might also provide a means to produce varied biological responses to structurally distinct ligands that act on the same receptor. In the case of the PTHR, such an effect could conceivably produce altered responses to PTH vs. PTHrP, and this might underlie the differing vitamin D-stimulating and bone-resorbing responses seen for PTH(1–34) and PTHrP(1–36) analogs in recent in vivo studies performed in humans (50, 51). The mechanisms involved here are still unclear.

In earlier studies performed in intact (52) or solubilized (53) membranes prepared from canine renal cortex, nonhydrolyzable GTP analogs were found to inhibit the binding of PTH(1–34) by approximately 75%; an extent considerably greater than that seen in our current studies performed in intact membranes prepared from cells transfected with the human PTHR (~25%). Although we have not assessed binding to the canine receptor, a likely explanation for the difference in GTP analog sensitivity seen in these studies is the difference in the species of receptor used (canine vs. human). The basis for this interpretation is that we have performed studies in membranes prepared from ROS 17/2.8 cells, which endogenously express the rat PTHR at a moderate level (~80,000 per cell), as well as in membranes prepared from COS-7 cells transfected to express the rat receptor at a much higher level (~2,000,000 per cell), and have found (data not shown) that, in both cases, GTP{gamma}S inhibits the binding of 125I-PTH(1–34) by approximately 75%, an extent similar to that seen in the earlier canine receptor studies. These findings raise the point that structural factors, such as the species of receptor or type of ligand analog used, might influence the extent to which the R0 state may form. The canine studies are of further interest in that they show that at least some R0 state can be detected for the PTHR in the more native milieu of renal cortical membranes.

Overall, our findings are consistent with the notion that the interaction of the amino-terminal agonist pharmacophore of PTH with the juxtamembrane region of the PTHR plays a major role in inducing the conformational changes in the receptor that lead to G protein coupling, and that, reciprocally, coupling of the PTHR to a heterotrimeric G protein containing G{alpha}S stabilizes the interaction of the amino-terminal pharmacophore of the ligand with the J domain of the receptor. Our findings make clear that the N domain of the receptor is not required for the formation of a high-affinity, G protein-coupled, agonist-receptor complex, yet is important for the formation of high-affinity complexes with PTH(1–34), and may be particularly relevant in cells where the receptor exists largely in a G protein-uncoupled state, such as in cells transfected to overexpress the PTHR. Given that PTH(1–34) can bind stably to a GTP{gamma}S-insensitive state of the PTHR, the availability of a PTH ligand that binds preferentially to a G protein-coupled, active conformation of the PTHR, as appears to be the case for [Aib1,3,M]PTH(1–15), could facilitate efforts to develop a small-molecule agonist ligand for the PTHR. Such a reagent could serve as a powerful new probe of the PTH-receptor interaction mechanism and might eventually lead to new therapeutic approaches for PTH-related diseases, such as osteoporosis.


   MATERIALS AND METHODS
TOP
 ABSTRACT
 INTRODUCTION
 RESULTS
 DISCUSSION
 MATERIALS AND METHODS
REFERENCES
 
Peptides and Reagents
All peptides used have been described by us previously (26, 27, 54) and were synthesized by the Protein and Peptide Core Facility at Massachusetts General Hospital (Boston, MA). The radioiodinated peptides, 125I-[Nle8,21,Tyr34]ratPTH(1–34)NH2, 125I-[Aib1,3,Nle8, Gln10,Har11,Ala12,Trp14,Tyr15]ratPTH(1–15)NH2 and 125I-[Ile5,Trp23,Tyr36]PTHrP(5–36)NH2, herein termed 125I-PTH(1–34), 125I-[Aib1,3,M]PTH(1–15) and 125I-PTHrP(5–36), respectively, were prepared using Na125I (specific activity: 2190 Ci/mmol; PerkinElmer/NEN Life Science Products, Boston, MA) and the oxidative chloramine-T procedure. Each radioligand was purified by reverse-phase HPLC to obtain an estimated specific activity of 2190 Cu/mmol.

Cell Culture
Cells were cultured in DMEM (Invitrogen Corp., Carlsbad, CA) supplemented with 10% fetal bovine serum (HyClone, Logan, UT), 100 U/ml penicillin G, and 100 µg/ml streptomycin, and maintained at 37 C (or 33 C as noted below) in a humidified atmosphere containing 5% CO2. The cell line HKRK-B7 is a clonal derivative of the porcine kidney cell line, LLC-PK1; these cells stably express the recombinant human PTHR at a cell surface density of approximately 950,000 receptors per cell (29). HKRK-B7 cells were harvested for membrane preparations 2–3 d after the cell monolayers became confluent. GnasE2–/E2– cells, herein termed G{alpha}S– cells, are a line of mouse embryonic fibroblasts that lack G{alpha}S due to homozygous disruption of exon 2 of the Gnas gene (34). Because these G{alpha}S– cells do not express detectable levels of endogenous PTHRs (34), they were infected with an adenoviral transduction vector (Invitrogen Corp.; multiplicity of infection = 100) into which was inserted a cDNA encoding the wild-type human PTHR (virus construction details available upon request). Parallel sets of cells were coinfected with this PTHR vector and a second adenovirus vector (multiplicity of infection = 100 for each virus), into which was inserted a cDNA encoding functional rat G{alpha}S. The cells were cultured at 33 C in six-well plates (6-cm diameter wells) and harvested for membrane preparation 2 d after infection. COS-7 cells were transiently transfected in six-well plates using Fugene-6 (Roche Diagnostics, Indianapolis, IN) and CsCl-purified plasmid DNA (3 µl Fugene, 1 µg DNA, per well). Human PTHR-encoding plasmids (pCDNA1 vector; Invitrogen Corp.) contained either the wild-type PTHR (55), PTHR-delNt, in which the segment Tyr23 (the amino terminus of the mature PTHR) to Arg181 (~10 amino acids amino-terminal of TM1) is replaced by an alanine (26), or the constitutively active mutant receptor, PTHR-H223R (32). To increase radioligand binding to PTHR-delNt, the COS-7 cells were cotransfected with a second plasmid (pcDNA1-Amp vector; Invitrogen Corp.) encoding the rat G{alpha}S mutant, G{alpha}S({alpha}3/ß5), in which five residues of the exposed {alpha}3/ß5 loop are replaced by the corresponding residues of rat G{alpha}i2 (N271K/K274D/R280K/T284D/I285T) (30). This mutant G{alpha}S has been shown to have increased capacity, relative to wild-type G{alpha}S, to stabilize receptor·G protein complexes (without increasing basal cAMP signaling), as shown for the ß2-adrenergic receptor (30), and the PTHR (12). Cotransfections were performed using 1 µg of each DNA and 6 µl of Fugene-6 per well of a six-well plate.

Cell Membrane Preparation
Cell monolayers in T175 flasks (HKRK-B7 cells) or six-well plates (COS-7 and G{alpha}S– cells) were washed with hypoosmotic lysis buffer [10 mM Tris-HCl (pH 7.8), 4 mM EDTA] and collected using a Teflon policeman in the same buffer supplemented with a protease inhibitor cocktail (final concentrations: 1 mM 4-(2-aminoethyl)benzenesulfonyl fluoride (AEBSF), 0.8 µM Aprotonin, 20 µM leupeptin, 40 µM Bestatin, 15 µM Pepstatin A, 14 µM E-64; Sigma-Aldrich Inc., St. Louis, MO). Three milliliters of this buffer were used for each T175 flask and 0.25 ml were used for each well of a six-well plate. The cells were then disrupted by passing 10 to 12 times through a steel ball-bearing/cylinder-based cell-shearing device (HGM Industries, Heidelberg, Germany) affixed at each end to a 10-ml syringe. The nuclei and cell fragments were removed by centrifugation at 800 x g for 10 min at 4 C, the membranes in the supernatant were collected by centrifugation at 14,000 x g for 30 min at 4 C, and the pellet was resuspended in membrane buffer [20 mM HEPES (pH 7.4), 0.1 M NaCl, 3 mM MgSO4, 20% glycerol, and the same protease inhibitor cocktail described above]. The membranes obtained from each T175 flask were resuspended in 1.0 ml of membrane buffer, and those from each well of a six-well plate were resuspended in 0.125 ml. The concentration of protein in the preparations was determined by the bicinchoninic acid protein detection system (Pierce, Rockford, IL) using BSA diluted in membrane buffer as a standard. Membrane aliquots (0.25 ml) were stored at –80 C and found to be stable at this temperature for at least 10 months.

Binding Assays
Binding reactions were performed at room temperature in assay buffer comprised of membrane buffer supplemented with BSA (3 mg/ml). Bound and free radioligand were separated by rapid vacuum filtration using 96-well vacuum filtration plates (Multiscreen-Durapore HV, low protein-binding, 0.65 µM membranes; Millipore Corp., Milford, MA) and a vacuum manifold. After rapid filtration of the sample and a single wash with 0.25 ml ice-cold assay buffer, the filters were air-dried, detached from the plate, and counted for {gamma} radioactivity in a {gamma} counter (Micromedic Model 600; Titertek Instruments, Huntsville, AL).

Binding Time Course Studies
Radioligand association and dissociation experiments were performed as bulk reactions in 15 ml round-bottom polystyrene snap-cap tubes (Falcon, Becton Dickinson, Franklin Lakes, NJ) in a total reaction volume of 3.0–5.0 ml. Reactions contained a total membrane protein concentration of 20–100 µg/ml, and a total radioactivity concentration of approximately 125,000 to 175,000 cpm/ml. Association reactions were initiated by the addition of membranes. At successive time-points thereafter, 0.2 ml aliquots (~25,000–35,000 cpm) were withdrawn and immediately processed by vacuum filtration, as described above. Nonspecific binding was determined for each radioligand in parallel reaction tubes containing an excess of the corresponding unlabeled ligand (1 x 10–6 M). For dissociation reactions, membranes and radioligand were preincubated for 90 min to allow complex formation. The dissociation phase was then initiated by the addition of a saturating concentration of the unlabeled ligand (1 x 10–6 M final concentration) with or without GTP{gamma}S (Sigma-Aldrich Inc., St. Louis, MO) at a final concentration of 5 x 10–5 M. Immediately before this addition (t = 0), and at successive time points thereafter, 0.2 ml aliquots were withdrawn and rapidly processed by vacuum filtration, as described above. Nonspecific binding was determined for each radioligand in parallel reaction tubes containing an excess of the corresponding unlabeled ligand (1 x 10–6 M) in both the formation and dissociation phases of the reaction. In both the association and dissociation reactions, nonspecific binding was found to be radioligand-dependent and to not vary over the time course of the reactions, nor between membrane/receptor preparations; accordingly, a time-averaged value of nonspecific binding was calculated in each experiment for each radioligand from the aggregate of nonspecific binding values obtained at each time point and thus used to calculate specific binding for that radioligand at each time point. The resulting values of specifically bound radioactivity were expressed as a percent of the maximum radioactivity specifically bound for the respective radioligand (determined by the curve-fitting routine described below for the association reactions and from the observed binding at t = 0 for the dissociation experiments).

Competition Binding Studies
Peptide competition and GTP{gamma}S inhibition reactions were incubated directly in the wells of the 96-well vacuum filtration plates. Each well contained a total volume of 230 µl, a total membrane protein concentration of 10–100 µg/ml and a total amount of radioactivity of approximately 30,000 cpm. Reagents were added and mixed in the wells using an eight-channel repeating pipettor. Reactions were incubated for 90 min, at the end of which the plate was applied to the vacuum manifold, the samples were filtered, the filters were washed once with 0.25 ml ice cold assay buffer, air-dried, detached from the plate and counted for {gamma} radioactivity. Nonspecific binding was determined for each radioligand in wells containing a saturating amount of unlabeled PTH ligand.

Data Calculations
Data were processed using least-squares, nonlinear regression analysis. Association time course data were analyzed using the mono-exponential equation: y = ymax·(1-e(–kobs·x)), where y is the radioactivity specifically bound, ymax is the maximum radioactivity specifically bound, x is time and kobs is the observed association rate constant. Dissociation time course data were analyzed using the biexponential decay equation: y = (span-1·e(–koff1·x))+(span-2·e(–koff2·x)), where span-1 and span-2 are the fractions of complexes with rapid (t1/2 ≤ 5 min) and slow (t1/2 > 5 min) dissociation rates, respectively; koff1 and koff2 are the corresponding dissociation rate constants (min–1); y is the specifically bound radioactivity and x is time. Values of t1/2 were calculated from the equation: t1/2 = 0.6932/k. Competition binding data were analyzed using the equation: y = ymin+(ymax – ymin)/1+(IC50/x)n, where y, ymin and ymax are the observed, calculated minimum and calculated maximum specific binding, respectively; x is inhibitor concentration (nM), IC50 is the concentration (nM) of inhibitor to achieve half of that inhibitor’s maximal effect and n is the slope factor (range: –0.8 to –1.4). Paired data sets were statistically compared using the Student’s t test (two-tailed) assuming unequal variances for the two sets.


   ACKNOWLEDGMENTS
 
We thank Catherine Berlot (Weis Center for Research, Danville, PA) for providing the G{alpha}S({alpha}3/ß5) expression plasmid.


   FOOTNOTES
 
This work was supported by Grant DK-11794 from the National Institutes of Health.

Disclosure: T.D., A.L., M.J.M., M.B., and H.J. have nothing to declare. T.J.G. and J.T.P. are recipients of a research grant from Chugai Pharmaceutical Co. of Japan; the grant is for the study of PTH ligands.

First Published Online December 8, 2005

Abbreviations: Aib, {alpha}-Amino-isobutyric acid; G protein, heterotrimeric ({alpha}ß{gamma}) guanine nucleotide-binding protein; G{alpha}S, stimulatory G protein {alpha} subunit that mediates activation of adenylyl cyclase; GPCR, G protein-coupled receptor; GTP{gamma}S, guanosine 5'-O-(3-thio)triphosphate; Har, homoarginine; J, juxtamembrane domain; N, amino-terminal extracellular domain; Nle, norleucine; PTHR, PTH/PTHrP receptor. PTHR-delNt, a PTHR construct that has most (mature amino terminus to Arg181) of the amino-terminal domain replaced by an alanine; PTHR-H223R, a constitutively active PTHR that contains the activating point mutation, His223->Arg; TM, one of the seven helical transmembrane domains of a GPCR.

Received for publication August 30, 2005. Accepted for publication November 28, 2005.


   REFERENCES
TOP
 ABSTRACT
 INTRODUCTION
 RESULTS
 DISCUSSION
 MATERIALS AND METHODS
 REFERENCES
 

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