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RECEPTORS AND SIGNAL TRANSDUCTION
1Department of Physiology and Biophysics and 2Neuroscience Program, University of Miami Miller School of Medicine, Miami, Florida; and 3Department of Biomedical Sciences, Colorado State University, Fort Collins, Colorado
Submitted 21 June 2005 ; accepted in final form 22 February 2006
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ABSTRACT |
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2 (i.e., cells that elevate [Ca2+]i in response to sweet, bitter, or umami stimuli). Taste transduction for sucrose is known to result in an elevation of both cAMP and calcium in taste buds. Thus we tested whether the cAMP increase in response to sucrose is a downstream consequence of calcium elevation. Even under conditions of depletion of stored and extracellular calcium, the cAMP response to sucrose stimulation persists in taste cells. The cAMP signal in response to monosodium glutamate stimulation is similarly unperturbed by calcium depletion. Our results suggest that tastant-evoked cAMP signals are not simply a secondary consequence of calcium modulation. Instead, cAMP and released Ca2+ may represent independent second messenger signals downstream of taste receptors. calcium-sensitive adenylyl cyclase; capacitative entry; cross talk; taste transduction
13 subunit appears to be taste specific and associated with G1 (14). This G113 dimer has been shown directly to activate a phospholipase C (PLC2), stimulating the production of inositol 1,4,5-trisphosphate (IP3) and eventually triggering an increase in cytoplasmic Ca2+ (14, 23, 35, 38). Strong support for this sequence of signaling events is derived from the pronounced taste deficit that results from genetic ablation of PLC2 (45). Although release of stored Ca2+ (triggered by PLC2 activity) is essential, taste-evoked calcium transients in taste cells may also include a component of capacitative entry from the extracellular medium (28). Despite the recent emphasis on this IP3-mediated calcium release pathway, there is evidence that changes in cAMP and cGMP concentration occur after tastant stimulation. Cyclic nucleotide modulation has been demonstrated after stimulation with some sweet, bitter, and umami stimuli (1, 39, 44), and exogenously applied cAMP appears to mimic tastant-evoked activity (8). Nevertheless, the significance and source of cAMP and cGMP in taste transduction are unclear, given the essential role of IP3-mediated signaling.
Cells can modulate cytoplasmic cAMP levels by regulating the function of cAMP-synthesizing adenylyl cyclases (ACs), cAMP-hydrolyzing phosphodiesterases (PDEs), or both. The membrane ACs are integral membrane proteins that comprise a family of nine isoforms, each with distinct regulatory properties. G protein-coupled receptors regulate ACs through G protein subunits such as the stimulatory G
s, the inhibitory Gi, or G dimers that exhibit heterogeneous functional interactions (12, 30). Various AC isoforms are also responsive to modulators such as calcium and calmodulin. Of these, our previous studies (1) demonstrated the presence of mRNA and protein for AC4, AC5/6, and AC8 in rat taste buds. AC5/6 and AC8 are all sensitive to calcium concentrations, based on in vitro assays; AC5 and 6 are inhibited (16), whereas AC8 is stimulated, by calcium (5). The presence of calcium-sensitive ACs in taste cells suggests that tastant-evoked cAMP synthesis might simply be a secondary consequence of the elevation of cytoplasmic calcium. Such interaction between the two pathways has been reported in neural tissue, in neurally derived pheochromocytoma PC12 cells, and in certain endocrine cells (4). In many neuronal cell types, AC activity is stimulated by physiological concentrations of Ca2+ on activation of the PLC pathway or activation of voltage-gated calcium channels (7, 19).
Here we demonstrate the functional presence of a calcium-stimulated AC in rat circumvallate (CV) taste buds. As with other excitable cell types, the calcium stimulation is dependent on entry from extracellular space rather than release from intracellular stores. We show that AC8 is localized in the same cells as PLC2 (a key enzyme for taste transduction) and investigate its role in sweet and glutamate taste. However, we demonstrate that although AC activity is enhanced by Ca2+ influx into taste cells, the cAMP response to tastants [sucrose and monosodium glutamate (MSG)] persists even in the absence of extracellular Ca2+. Our results suggest that the cAMP signal for these tastants is a direct outcome of receptor activation, rather than simply a downstream consequence of the elevation of cytoplasmic Ca2+ levels following activation of PLC2.
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MATERIALS AND METHODS |
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Reagents and solutions. Formulations for physiological saline solutions were as follows: Tyrode buffer (mM: 140 NaCl, 5 KCl, 2 CaCl2, 1 MgCl2, 10 HEPES, 10 glucose, 10 sodium pyruvate, pH 7.4); Ca2+- and Mg2+-free (CMF) Tyrode buffer (mM: 140 NaCl, 5 KCl, 2 EGTA, 10 HEPES, 10 glucose, 10 sodium pyruvate, pH 7.4); phosphate-buffered saline (PBS; mM: 154 NaCl, 1 KH2PO4, 3 Na2HPO4, pH 7.4). The following reagents were purchased from Sigma (St. Louis, MO) and were dissolved in dimethyl sulfoxide: forskolin (Fsk) at 20 mM; 3-isobutyl-1-methylxanthine (IBMX) at 500 mM; cycloheximide at 100 mg/ml; thapsigargin and calcimycin (A-23187) at 1 mM. Aliquots of each were stored at –20°C and were freshly diluted into Tyrode buffer for each experiment. Fsk, IBMX, thapsigargin, and A-23187 were used at concentrations within twofold of published EC50 values. Taste stimuli were diluted into Tyrode buffer at concentrations that are taste effective and shown previously to elicit taste-specific cAMP signals (1, 39).
cAMP measurements.
Rat CV or nontaste epithelial sheets were cut in the midline to yield two equal halves, which served as paired control and treated samples. Pairs of epithelial sheets were subjected to stimulation paradigms as shown in Figs. 1
and 3 and described below. The supernatant solutions were then removed and replaced with 16% HClO4 in Tyrode buffer, and tissues were extracted by vortexing and freezing at –80°C. Subsequent steps for neutralization and clarification of the extract were according to Krizhanovsky et al. (18), and cAMP was quantified with an enzyme immunoassay kit (Amersham Biosciences, Piscataway, NJ) as reported previously (1). To measure protein levels in tissues, we first hydrolyzed them in 5 N NaOH (100 µl for CV samples; 500 µl for nontaste samples) at 60°C for 3 h. Aliquots (10 µl) of the hydrolysates were neutralized with 190 µl of 1 M Tris·HCl (pH 7.0) and assayed with a Nano-Orange Protein Quantitation Kit (Molecular Probes, Eugene, OR). Paired two-tailed t-test was performed with Prism (version 4.00, GraphPad Software, San Diego CA).
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2 (1:4,000), both from Santa Cruz Biotechnology (Santa Cruz, CA). Secondary antibodies (Molecular Probes) used for detection were donkey anti-goat IgG-Alexa 488 (1:1,000) for AC8 and donkey anti-rabbit IgG-Alexa 594 (1:1,000) for PLC2. Fluorescence images were captured on an Olympus Fluoview scanning confocal microscope. We previously confirmed (1) by immunoblot that the anti-AC8 antibody reacts against an antigen of the appropriate size in brain membrane extracts. The specificity for the AC8 antibody was further confirmed by preincubation with the corresponding blocking peptide (Santa Cruz Biotechnology). The specificity of the PLC2 antibody was confirmed in parallel by immunostaining sections of taste papillae from PLC2-knockout mice; no fluorescence was detected. Functional imaging. CV papillae were loaded with calcium green-dextran, cut into 100-µm-thick slices, and functionally imaged for Ca2+ exactly as previously described (33). Imaging was carried out with argon laser excitation (488 nm) and an FITC filter set to scan >3.5-µm-thick optical sections once every 1.1 s. Taste stimuli were focally and transiently applied to the vicinity of the taste pore. The concentration of tastant reaching the taste pore was estimated by monitoring the dilution of a fluorescent indicator dye included in the stimulation pipette. Recordings are displayed as change of fluorescence normalized to initial fluorescence. It should be noted that this measurement yields relative changes in Ca2+ concentration rather than the absolute concentrations of Ca2+ found within cells.
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RESULTS |
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Thapsigargin treatment in many cells induces capacitative entry of Ca2+ across the plasma membrane (32). We asked whether the above stimulation of AC activity resulted directly from the release of stored Ca2+ or was dependent on a secondary (capacitative) Ca2+ influx. Paired halves of taste bud-containing CV epithelium were pretreated with 10 µM Fsk in Tyrode solution (containing 2 mM Ca2+) for 1 min. One piece of taste epithelium (control) was then bathed in 10 µM Fsk in CMF Tyrode buffer. The other paired sample was bathed in 10 µM forskolin + 5 µM thapsigargin in CMF Tyrode buffer. Both tissue samples were incubated for one additional minute (see schematic, Fig. 1B). Thapsigargin failed to elevate cAMP levels when it was applied in a calcium-free condition; cAMP levels in treated samples were 99 ± 9% (n = 8) of those in control samples. The result suggests that the thapsigargin-induced stimulation of AC activity depends on Ca2+ entry across the plasma membrane, which would be lacking in the present paradigm. We noted the high animal-to-animal variability in cAMP levels in the short-term calcium-free condition. Taste buds transferred to an extracellular buffer devoid of calcium often exhibit unstable fluctuations of cytoplasmic Ca2+ (Ref. 28; unpublished observations in our laboratories). Perhaps the variability of cAMP relates to such fluctuations, but our data do not directly address this. Nevertheless, CV taste epithelia tested in pairs derived from individual animals show that thapsigargin fails to elevate cellular cAMP in the absence of extracellular calcium.
We also tested the ability of 3 µM A-23187, a calcium ionophore, when applied in Tyrode solution (i.e., with 2 mM extracellular Ca2+), to stimulate AC activity in taste buds (Fig. 1C). The cAMP concentration in A-23187-treated samples, as a percentage of control, was 154 ± 8%, similar to the effect of 5 µM thapsigargin. Parallel stimulations of nontaste epithelial sheets under all three conditions of calcium modulation showed no evidence of enhanced AC activity (see Fig. 1).
Immunolocalization of calcium-stimulated AC8 in taste cells.
The above results demonstrate that taste buds contain a calcium-stimulated AC that is dependent on Ca2+ entry rather than release from intracellular stores. When taste receptor cells are stimulated with many tastants, receptor-activated PLC2 causes the release of Ca2+ from intracellular stores (3, 14, 45). In addition, during taste stimulation, there is evidence of Ca2+ entry across the plasma membrane, through capacitative or voltage-gated mechanisms (3, 28, 31). Hence, we examined whether the calcium-sensitive AC of taste cells is expressed in the same cells that undergo calcium dynamics triggered by tastants.
Earlier, we showed (1) that of the two known calcium-stimulated AC isoforms only AC8 is expressed in rodent taste buds. Hence, we carried out immunocytochemistry to determine whether AC8 is found in cells that exhibit Ca2+ mobilization and Ca2+ entry in response to taste stimuli. In taste buds, cells that express the G protein-coupled taste receptors also express the effector enzyme PLC2 (6). Using a well-characterized antibody against PLC2, we found robust staining in a large subset of taste cells in CV (Fig. 2B) and foliate papillae from both rats and mice. Generally, immunoreactivity was displayed throughout the cytoplasm of labeled cells (Fig. 2F). Immunoreactivity was specific to taste buds and was not present in the lingual epithelium surrounding taste buds. To confirm the specificity of immunoreactivity, we also immunostained sections of CV papillae from PLC2-knockout mice (15). As expected, no immunofluorescence was detected in any taste buds (Fig. 2I) or elsewhere in this tissue. Additional controls for immunofluorescence microscopy consisted of omitting the primary antibody and preincubating the primary antibody with its corresponding antigenic peptide before application; each of these controls consistently yielded no staining (not shown).
Immunoreactivity for AC8 was also detected in a subset of taste cells that were broad and had rounded, large nuclei (Fig. 2A). Fluorescence was concentrated in the cytoplasm, whereas nuclei were devoid of staining. We noted that in some AC8-immunopositive cells staining was concentrated in the apical portion of the cell. In most cells, AC8 reactivity was distributed unevenly as patches. Very similar immunostaining patterns were also observed in rat foliate, mouse CV, and mouse foliate papillae. When anti-AC8 was preincubated with antigenic peptide before application on tissue sections, all immunofluorescence was lost (Fig. 2, J and K).
To quantify the coexpression of these two genes, we scored immunopositive cells that were well defined, with visible nuclei. We counted all such cells within taste buds in both crypts of one section of a CV papilla from each of three rats. Out of 146 cells positive for AC8, 119 cells were also strongly positive for PLC2 (79 ± 5% across 3 animals). Conversely, of 390 cells positive for PLC2, 119 cells were also strongly positive for AC8 (33 ± 8% across 3 animals). We also scored taste buds from one immunolabeling experiment using mouse CV papillae and detected a frequency of coexpression of AC8 and PLC2 similar to that in the rat.
Effect of calcium on tastant-evoked cAMP modulation.
Because the majority of AC8-positive cells also express PLC2, a key marker of taste transduction, we examined whether there is a relation between calcium-sensitive AC activity and taste signaling. Increases of cAMP have been noted in response to sweet taste stimuli (39) and decreases in response to umami and bitter (1, 44) stimuli. Control stimulations using sweet taste blockers or nonumami analogs previously confirmed that in both sweet and umami the cAMP signals are taste related and not simply responses to osmotic perturbations (1, 39). The mechanism for altering cAMP after sweet or umami has not been explored and was the focus of the following set of experiments. Although bitter tastants also modulate cyclic nucleotides, these signals are very transient (<1 s) (18, 44) and hence are not amenable to the present method of analysis.
When taste buds are stimulated with sweet or umami tastants, there is release of stored Ca2+ (3, 24, 26) and the subsequent capacitative entry of Ca2+ (28). This suggests two alternative sources for the cAMP signals reportedly evoked by tastants. First, G proteins might directly activate or inhibit ACs or PDEs (Gs, Gi or Ggustducin, respectively). Alternatively, calcium (released or entering capacitatively) might secondarily modulate a calcium-sensitive AC.
To distinguish between these alternatives, we carried out sucrose stimulation under normal physiological conditions, as well as under conditions of depleted Ca2+. We first identified conditions under which stores of cytoplasmic Ca2+ are depleted. Using a well-established paradigm, we imaged the calcium response of CV taste cells to focal application of the bitter tastant cycloheximide. As expected, a pronounced elevation of cytoplasmic Ca2+ was observed on application of 100 µM cycloheximide (Fig. 3A, left). The CV slice was then bathed in CMF Tyrode buffer for 20 min and was restimulated with 100 µM cycloheximide. The absence of a detectable Ca2+ response (Fig. 3A, middle) suggested that cytoplasmic Ca2+ stores had been depleted. Replenishment of stores, as evidenced by the recovery of a calcium response to cycloheximide, was achieved by bathing the slice in regular Tyrode buffer for 30 min (Fig. 3A, right).
Paired halves of CV epithelium in Tyrode solution were stimulated with either 0.3 mM IBMX + 500 mM sucrose for 6 min or 0.3 mM IBMX alone as a control. A substantial accumulation of cAMP resulted from sucrose stimulation (cAMP concentration for sucrose, as a percentage of control, was 244 ± 28%). These data are consistent with those previously reported (39). We then repeated this stimulation paradigm under conditions established above wherein calcium was lacking both in stores and in the extracellular milieu. Paired CV samples were preincubated in CMF Tyrode solution for 15–20 min and were stimulated with 0.3 mM IBMX with or without 500 mM sucrose in CMF Tyrode solution. Even in the absence of Ca2+ release or Ca2+ entry (Fig. 3C), sucrose-stimulated samples showed an increase in cAMP (cAMP concentration for sucrose, as a percentage of control, was 224 ± 10%).
We also considered that the decrease of cAMP previously reported (1) for umami stimulation could result from a calcium-inhibited tonic AC activity. To investigate this possibility, we carried out MSG stimulations under calcium-replete and calcium-depleted conditions. Paired halves of CV epithelium in Tyrode solution were treated with either 0.3 mM IBMX (control) or 0.3 mM IBMX + 20 mM MSG, both for 6 min at 30°C. The results (Fig. 3B) showed a decrease in cAMP induced by MSG (cAMP concentration for MSG, as a percentage of control, was 71 ± 7%), consistent with our previous observations (1). To assess whether modulation of cAMP is a downstream consequence of calcium signaling after umami stimulation, we repeated the MSG stimulation with calcium depleted from stores and extracellular medium. As shown in Fig. 3C, MSG elicited a decrease in cAMP concentration even under conditions that prevent Ca2+ release or entry (cAMP concentration for MSG, as a percentage of control, was 66 ± 7%).
As a further test of the independence of the taste-evoked cAMP and Ca2+ signals, we carried out taste stimulation in the presence of 5 µM U-73122, an inhibitor of PLC (41). Taste epithelium was pretreated with the drug for 15 min before application of IBMX and sucrose. The paradigm was essentially similar to that shown in Fig. 3C except that cells were in normal, not CMF, Tyrode solution. Sucrose-stimulated samples exhibited an increase of cAMP concentration (201 ± 6%; P = 0.003, n = 3) over the unstimulated controls (Fig. 3D). Similarly, MSG-stimulated samples exhibited a pronounced decrease of cAMP concentration (75 ± 2%; P = 0.01, n = 3). In contrast, in calcium imaging experiments, 5 µM U-73122 was almost completely effective at blocking the tastant-evoked calcium transient (not shown).
The cAMP responses to both sucrose and MSG were taste specific. None of the foregoing taste stimulations, either in the presence or in the absence of Ca2+, resulted in any significant alteration of cAMP levels between paired samples of nontaste lingual epithelium (see Fig. 3).
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DISCUSSION |
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113 subunits, trigger the synthesis of IP3 and the release of stored Ca2+ (14, 36, 44). This IP3-mediated Ca2+ release also occurs when taste buds are stimulated with sweet or umami compounds (3, 24, 26). Tastant-mediated Ca2+ release (shown for denatonium, a bitter tastant) is thought to be coupled to a concurrent entry of Ca2+ from extracellular space, via capacitative channels (28). PLC2 is a marker for taste cells that exhibit Ca2+ release and, potentially, capacitative Ca2+ entry in response to tastants. Here we have shown that AC8 is predominantly expressed in this same population of tastant-responsive cells. Nevertheless, we found that tastant-mediated changes in cAMP levels were not perturbed when we altered the availability of Ca2+ for release or capacitative entry.
There are two possible explanations for this apparent conundrum. First, it is possible that AC8 (which is expressed in only a subset of PLC2-positive cells) is present only in nonsweet, nonumami cells. We note that capacitative entry has been demonstrated only for bitter, not sweet or umami, tastants (28). Second, AC8 in taste cells may be localized in cellular microdomains distinct from those for taste receptors. Hence, if taste receptors are apically located and if Ca2+ diffusion is tightly restricted, as it is in most neurons, AC8 may not be subjected to capacitative Ca2+ entry during taste stimulation. However, during thapsigargin treatment, intracellular Ca2+ increases globally across the cell, which would impact ACs sequestered in other microdomains. Other types of receptors found on taste cells, e.g., muscarinic (27), purinergic (2), or cholecystokinin (13) receptors, all of which activate PLC signaling, might be the physiological triggers for AC8 activity.
Our results suggest that the positive or negative cAMP signals that we and others have reported for tastants are not simply a downstream consequence of Ca2+ mobilization after taste stimulation. Instead, we propose that downstream of taste receptors two parallel and independent G protein-triggered pathways are activated. The G arm stimulates PLC2 and results in calcium elevation. The G arm may trigger cAMP modulation via the action of Gs, Gi, or Ggustducin, each of which is expressed in taste buds (20, 23, 25). Specifically, Gs, a subunit that stimulates all ACs, may give rise to increases of cAMP (for sucrose). Decreases of cAMP (for bitter and umami stimuli) may arise from activation of Gi to inhibit AC or Ggustducin to activate PDEs.
What are the downstream consequences of cAMP modulation in taste cells? Decreases in cellular cAMP may affect taste transduction by modulating the sensitivity of the PLC pathway. For instance, cAMP-mediated phosphorylation is known to decrease the activity of both PLC2 (22) and IP3R3 (11), the IP3 receptor located on taste cell stores (6). Thus we postulate that decreased intracellular cAMP levels following umami stimulation may diminish phosphorylation of PLC2 and IP3R3, thereby prolonging the Ca2+ transient. Consistent with this hypothesis, membrane-permeant analogs of cAMP blocked the electrophysiological and Ca2+ responses to umami stimuli in rat fungiform taste cells (21).
In the case of sweet transduction, the central role of cAMP is less clear. In hamsters, membrane-permeant analogs of cAMP and cGMP mimic the trains of action potentials elicited by sweet stimuli (8). Patch clamp recordings in frogs and hamsters indicate that cyclic nucleotides depolarize sweet-responsive taste cells by blocking a K+ current (9), possibly by direct action on the channel (17, 42). These data are difficult to reconcile with the seemingly exclusive role of PLC2-mediated calcium release suggested by studies on PLC2-knockout mice (45). A solution to this conundrum may lie in the presence of two second messenger pathways triggered by sweeteners, (G-mediated Ca2+ modulation and G-stimulated cAMP modulation). Indeed, convergence of calcium and cyclic nucleotide pathways onto a common target K+ channel has been demonstrated in the hamster (42). We postulate that the relative importance of these two pathways may differ between mice (in which the G pathway predominates) and rats or hamsters (in which the G pathway is prominent). It is important to note that, even in the mouse, the impact of cyclic nucleotide signaling is evidenced by the decrease in behavioral and neural responses to sweet, bitter, and umami stimuli when gustducin is knocked out (34, 37, 43). Further studies using single-cell approaches will be required to resolve the specific roles of these two signaling pathways in sweet transduction.
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ACKNOWLEDGMENTS |
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FOOTNOTES |
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The costs of publication of this article were defrayed in part by the payment of page charges. The article must therefore be hereby marked "advertisement" in accordance with 18 U.S.C. Section 1734 solely to indicate this fact.
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REFERENCES |
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|---|
2. Baryshnikov SG, Rogachevskaja OA, and Kolesnikov SS. Calcium signaling mediated by P2Y receptors in mouse taste cells. J Neurophysiol 90: 3283–3294, 2003.
3. Bernhardt SJ, Naim M, Zehavi U, and Lindemann B. Changes in IP3 and cytosolic Ca2+ in response to sugars and non-sugar sweeteners in transduction of sweet taste in the rat. J Physiol 490: 325–336, 1996.
4. Caldwell KK, Boyajian CL, and Cooper DMF. The effects of Ca2+ and calmodulin on adenylyl cyclase activity in plasma membranes derived from neural and nonneural cells. Cell Calcium 13: 107–121, 1992.[CrossRef][Web of Science][Medline]
5. Cali JJ, Zwaagstra JC, Mons N, Cooper DMF, and Krupinski J. Type VIII adenylyl cyclase. A Ca2+/calmodulin-stimulated enzyme expressed in discrete regions of rat brain. J Biol Chem 269: 12190–12195, 1994.
6. Clapp TR, Stone LM, Margolskee RF, and Kinnamon SC. Immunocytochemical evidence for co-expression of Type III IP3 receptor with signaling components of bitter taste transduction. BMC Neurosci 2: 6, 2001.[CrossRef][Medline]
7. Cooper DM. Molecular and cellular requirements for the regulation of adenylate cyclases by calcium. Biochem Soc Trans 31: 912–915, 2003.[Web of Science][Medline]
8. Cummings TA, Powell J, and Kinnamon SC. Sweet taste transduction in hamster taste cells: evidence for the role of cyclic nucleotides. J Neurophysiol 70: 2326–2336, 1993.
9. Cummings TA, Daniels C, and Kinnamon SC. Sweet taste transduction in hamster: sweeteners and cyclic nucleotides depolarize taste cells by reducing a K+ current. J Neurophysiol 75: 1256–1263, 1996.
10. Gilbertson TA, Roper SD, and Kinnamon SC. Proton currents through amiloride-sensitive Na+ channels in isolated hamster taste cells: enhancement by vasopressin and cAMP. Neuron 10: 931–942, 1993.[CrossRef][Web of Science][Medline]
11. Giovannucci DR, Groblewski GE, Sneyd J, and Yule DI. Targeted phosphorylation of inositol 1,4,5-trisphosphate receptors selectively inhibits localized Ca2+ release and shapes oscillatory Ca2+ signals. J Biol Chem 275: 33704–33711, 2000.
12. Hanoune J and Defer N. Regulation and role of adenylyl cyclase isoforms. Annu Rev Pharmacol Toxicol 41: 145–174, 2001.[CrossRef][Web of Science][Medline]
13. Herness S, Zhao FL, Lu SG, Kaya N, and Shen T. Expression and physiological actions of cholecystokinin in rat taste receptor cells. J Neurosci 22: 10018–10029, 2002.
14. Huang L, Shanker YG, Dubauskaite J, Zheng JZ, Yan W, Rosenzweig S, Spielman AI, Max M, and Margolskee RF. G13 colocalizes with gustducin in taste receptor cells and mediates IP3 responses to bitter denatonium. Nat Neurosci 2: 1055–1062, 1999.[CrossRef][Web of Science][Medline]
15. Jiang H, Kuang Y, Wu Y, Xie W, Simon MI, and Wu D. Roles of phospholipase C2 in chemoattractant-elicited responses. Proc Natl Acad Sci USA 94: 7971–7975, 1997.
16. Katsushika S, Chen L, Kawabe JI, Nilakantan R, Halnon NJ, Homcy CJ, and Ishikawa Y. Cloning and characterization of a sixth adenylyl cyclase isoform: types V and VI constitute a subgroup within the mammalian adenylyl cyclase family. Proc Natl Acad Sci USA 89: 8774–8778, 1992.
17. Kolesnikov SS and Margolskee RF. A cyclic-nucleotide-suppressible conductance activated by transducin in taste cells. Nature 376: 85–88, 1995.[CrossRef][Medline]
18. Krizhanovsky V, Agamy O, and Naim M. Sucrose-stimulated subsecond transient increase in cGMP level in rat intact circumvallate taste bud cells. Am J Physiol Cell Physiol 279: C120–C125, 2000.
19. Krsmanovic LZ, Mores N, Navarro CE, Tomic M, and Catt KJ. Regulation of Ca2+-sensitive adenylyl cyclase in gonadotropin-releasing hormone neurons. Mol Endocrinol 15: 429–440, 2001.
20. Kusakabe Y, Yasuoka A, Asano-Miyoshi M, Iwabuchi K, Matsumoto I, Arai S, Emori Y, and Abe K. Comprehensive study on G protein -subunits in taste bud cells, with special reference to the occurrence of Gi2 as a major G species. Chem Senses 25: 525–531, 2000.
21. Lin W, Ogura T, and Kinnamon SC. Responses to di-sodium guanosine 5'-monophosphate and monosodium L-glutamate in taste receptor cells of rat fungiform papillae. J Neurophysiol 89: 1434–1439, 2003.
22. Liu MY and Simon MI. Regulation by cAMP-dependent protein kinase of a G-protein-mediated phospholipase C. Nature 382: 83–87, 1996.[CrossRef][Medline]
23. Margolskee RF. Molecular mechanisms of bitter and sweet taste transduction. J Biol Chem 277: 1–4, 2002.
24. Maruyama Y, Pereira E, Margolskee RF, Chaudhari N, and Roper SD. Umami responses in mouse taste cells indicate more than one receptor. J Neurosci 26: 2227–2234, 2006.
25. McLaughlin SK, McKinnon PJ, and Margolskee RF. Gustducin is a taste-cell-specific G protein closely related to the transducins. Nature 357: 563–569, 1992.[CrossRef][Medline]
26. Nakashima K and Ninomiya Y. Increase in inositol 1,4,5-triphosphate levels of the fungiform papilla in response to saccharin and bitter substances in mice. Cell Physiol Biochem 8: 224–230, 1998.[CrossRef][Web of Science][Medline]
27. Ogura T. Acetylcholine increases intracellular Ca2+ in taste cells via activation of muscarinic receptors. J Neurophysiol 87: 2643–2649, 2002.
28. Ogura T, Margolskee RF, and Kinnamon SC. Taste receptor cell responses to the bitter stimulus denatonium involve Ca2+ influx via store-operated channels. J Neurophysiol 87: 3152–3155, 2002.
29. Oshikawa J, Toya Y, Fujita T, Egawa M, Kawabe J, Umemura S, and Ishikawa Y. Nicotinic acetylcholine receptor 7 regulates cAMP signal within lipid rafts. Am J Physiol Cell Physiol 285: C567–C574, 2003.
30. Patel TB, Du Z, Pierre S, Cartin L, and Scholich K. Molecular biological approaches to unravel adenylyl cyclase signaling and function. Gene 269: 13–25, 2001.[CrossRef][Web of Science][Medline]
31. Perez CA, Huang L, Rong M, Kozak JA, Preuss AK, Zhang H, Max M, and Margolskee RF. A transient receptor potential channel expressed in taste receptor cells. Nat Neurosci 5: 1169–1176, 2002.[CrossRef][Web of Science][Medline]
32. Putney JW Jr. Capacitative calcium entry revisited. Cell Calcium 11: 611–624, 1990.[CrossRef][Web of Science][Medline]
33. Richter TA, Caicedo A, and Roper SD. Sour taste stimuli evoke Ca2+ and pH responses in mouse taste cells. J Physiol 547: 475–483, 2003.
34. Rong M, He W, Yasumatsu K, Kokrashvili Z, Perez CA, Mosinger B, Ninomiya Y, Margolskee RF, and Damak S. Signal transduction of umami taste: insights from knockout mice. Chem Senses 30: i33–i34, 2005.
35. Rossler P, Kroner C, Freitag J, Noe J, and Breer H. Identification of a phospholipase C beta subtype in rat taste cells. Eur J Cell Biol 77:253–261, 1998.[Web of Science][Medline]
36. Rössler P, Boekhoff I, Tareilus E, Beck S, Breer H, and Freitag J. G protein complexes in circumvallate taste cells involved in bitter transduction. Chem Senses 25: 413–421, 2000.
37. Ruiz CJ, Wray K, Delay ER, and Kinnamon SC. Behavioral evidence for a role of -gustducin in umami taste. Chem Senses 28: 573–579, 2003.
38. Spielman AI, Huque T, Nagai H, Whitney G, and Brand JG. Generation of inositol phosphates in bitter taste transduction. Physiol Behav 56: 1149–1155, 1994.[CrossRef][Medline]
39. Striem BJ, Naim M, and Lindemann B. Generation of cyclic AMP in taste buds of the rat circumvallate papilla in response to sucrose. Cell Physiol Biochem 1: 46–54, 1991.
40. Thastrup O, Cullen PJ, Drobak BK, Hanley MR, and Dawson AP. Thapsigargin, a tumor promoter, discharges intracellular Ca2+ stores by specific inhibition of the endoplasmic reticulum Ca2+-ATPase. Proc Natl Acad Sci USA 87: 2466–2470, 1990.
41. Thompson AK, Mostafapour SP, Denlinger LC, Bleasdale JE, and Fisher SK. The aminosteroid U-73122 inhibits muscarinic receptor sequestration and phosphoinositide hydrolysis in Sk-N-Sh neuroblastoma cells. J Biol Chem 266: 23856–23862, 1991.
42. Varkevisser B and Kinnamon SC. Sweet taste transduction in hamster: role of protein kinases. J Neurophysiol 83: 2526–2532, 2000.
43. Wong GT, Gannon KS, and Margolskee RF. Transduction of bitter and sweet taste by gustducin. Nature 381: 796–800, 1996.[CrossRef][Medline]
44. Yan W, Sunavala G, Rosenzweig S, Dasso M, Brand JG, and Spielman AI. Bitter taste transduced by PLC-2-dependent rise in IP3 and -gustducin-dependent fall in cyclic nucleotides. Am J Physiol Cell Physiol 280: C742–C751, 2001.
45. Zhang Y, Hoon MA, Chandrashekar J, Mueller KL, Cook B, Wu D, Zuker CS, and Ryba NJ. Coding of sweet, bitter, and umami tastes: different receptor cells sharing similar signaling pathways. Cell 112: 293–301, 2003.[CrossRef][Web of Science][Medline]
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