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Regulation of TRPP3 Channel Function by N-terminal Domain Palmitoylation and Phosphorylation*

Transient receptor potential polycystin-3 (TRPP3) is a cation channel activated by calcium and proton and is involved in hedgehog signaling, intestinal development, and sour tasting. How TRPP3 channel function is regulated remains poorly understood. By N-terminal truncation mutations, electrophysiology, and Xenopus oocyte expression, we first identified fragment Asp-21–Ser-42 to be functionally important. We then found that deletion mutant Δ1–36 (TRPP3 missing fragment Met-1–Arg-36) has a similar function as wild-type TRPP3, whereas Δ1–38 is functionally dead, suggesting the importance of Val-37 or Cys-38. Further studies found that Cys-38, but not Val-37, is functionally critical. Cys-38 is a predicted site of palmitoylation, and indeed TRPP3 channel activity was inhibited by palmitoylation inhibitor 2-bromopalmitate and rescued by palmitoylation substrate palmitic acid. The TRPP3 N terminus (TRPP3NT, Met-1–Leu-95) localized along the plasma membrane of HEK293 cells but stayed in the cytoplasm with 2-bromopalmitate treatment or C38A mutation, indicating that TRPP3NT anchors to the surface membrane through palmitoylation at Cys-38. By acyl-biotin exchange assays, we showed that TRPP3, but not mutant C38A, is indeed palmitoylated. When putative phosphorylation sites near Cys-38 were mutated to Asp or Glu to mimic phosphorylation, only T39D and T39E reduced TRPP3 function. Furthermore, TRPP3NT displayed double bands in which the upper band was abolished by λ phosphatase treatment or T39A mutation. However, palmitoylation at Cys-38 and phosphorylation at Thr-39 independently regulated TRPP3 channel function, in contrast to previous reports about correlated palmitoylation with a proximate phosphorylation. Palmitoylation at Cys-38 represents a novel mechanism of functional regulation for TRPP3.

Transient receptor potential (TRP) 4 channels are a superfamily of cation channels that play distinct sensory roles in response to a variety of extracellular stimuli, including light, sound, chemicals, temperature, and touch (1). The TRP superfamily has been divided into the following eight subfamilies named after the first identified member in each subfamily: TRPC, TRPV, TRPM, TRPA, TRPN, TRPY, TRPML, and TRP polycystin. Similar to voltage-gated potassium channels, TRP channels were predicted to function as tetramers in which each subunit has six transmembrane helices (TM1-TM6), with a pore loop between TM5 and TM6, and cytosolic N and C termini of varying sizes (2). This structural architecture was confirmed by recently published TRPV1, -2, -6 and TRPA1 structures (3)(4)(5)(6).
The founding member of the TRP polycystin subfamily, TRPP2 (also called PKD2 or polycystin-2), is mutated in 15% autosomal dominant polycystic kidney disease (ADPKD), the most common genetic disorder of the kidney, affecting 1 in 400 to 1000 individuals worldwide (7). The remaining ADPKD is caused by mutations in the PKD1 gene. TRPP3, also called PKD2L1 or polycystin-L, is a homologue of TRPP2 with 50% identity in protein sequence but is not involved in ADPKD. TRPP3 is expressed in bipolar neurons in the tongue taste buds where it presumably plays an important role in sour tastes. Genetic ablation of cells expressing TRPP3 eliminates gustatory nerve response to sour stimuli in mice (8 -10). Involvement of TRPP3 in tasting sour was later supported by the report that TRPP3 knock-out mice display a defective ability for tasting acid (11). TRPP3 is expressed in neurons surrounding the central canal of spinal cord where it may be implicated in modulating pH-dependent action potential characteristics (8,12,13). TRPP3 is also expressed in brain, kidney, and heart with unknown function (14).
TRPP3 is localized on the surface membrane and/or endoplasmic reticulum membrane, in part depending on the cell type. In Xenopus laevis oocytes, TRPP3 targets to the plasma membrane when expressed alone and acts as a Ca 2ϩ -activated channel permeable to Na ϩ , K ϩ , and Ca 2ϩ (15,16). In human embryonic kidney (HEK) cell lines, TRPP3 mainly targets to the endoplasmic reticulum membrane when expressed alone but traffics to the plasma membrane when co-expressed with PKD1 or PKD1L3, a homologue of PKD1 (9,17,18). TRPP3 alone, or together with PKD1L3, mediates pH-dependent cation conductance in an off-response manner, i.e. activation occurred only after low extracellular pH was removed (9,19,53). TRPP3 was also found to be expressed in primary cilium and to regulate ciliary Ca 2ϩ concentration and hedgehog signaling (20,21). Although TRPP3 contains putative phosphorylation, glycosylation, and palmitoylation sites, it is unclear whether and how it is regulated via post-translational modifications. Its homologue TRPP2 channel activity or trafficking was reported to be regulated by phosphorylation at C-terminal Ser-812 by casein kinase II (22) and N-terminal Ser-76 by glycogen synthase kinase 3 (23). Moreover, TRPP2 is also glycosylated but with an unclear functional role (24).
Palmitoylation is a reversible covalent fatty acid modification that attaches the C16 fatty acid palmitate to a cytoplasmic cysteine residue (25). Like other lipid modifications, such as myristoylation and prenylation, palmitoylation serves to tether cytoplasmic proteins to the surface of membranes. In mammals, there are 23 palmitoyltransferases containing a conserved zinc-binding site and Asp-His-His-Cys (DHHC) motif; thus, these enzymes are often referred to as zDHHC-palmitoyltransferases (26,27). The reversibility of the palmitoylation reaction represents a dynamic regulation mechanism. In some membrane proteins, such as G-protein coupled receptors, palmitoylation of a C-terminal domain has led to the formation of an additional intracellular loop linked to receptor de-sensitization (28 -30). An increasing number of ion channel proteins has been reported to undergo palmitoylation as a way of controlling the anchorage of an intracellular domain to membranes (31). An interplay between palmitoylation and phosphorylation has recently been recognized as a new mechanism of regulating the trafficking or function of ion channels (31). Among them, TRPML1 has been reported to undergo palmitoylation and de-phosphorylation, following histamine stimulation of gastric acid secretion, which may underlie the mechanism of its endocytosis (32,33).
In this study, using X. laevis oocyte expression and the twoelectrode voltage clamp (TEVC) technique, we first identified the N-terminal residue Cys-38 in human TRPP3 to be critical for its channel function. We then showed that this is mediated through palmitoylation at Cys-38. We also identified Thr-39 to be a functionally important phosphorylation site immediately downstream of Cys-38. Finally, we showed that palmitoylation at Cys-38 and phosphorylation at Thr-39 regulate TRPP3 channel function rather independently, in contrast to other ion channels that are regulated by palmitoylation and correlated phosphorylation at a proximate residue.

Identification of TRPP3 N-terminal Cys-38 Important for Its
Channel Function-Our previous report showed the importance of the N terminus of TRPP3 (TRPP3NT, Met-1-Leu-95) for its Ca 2ϩ -activated channel activity when expressed in Xenopus oocytes (16). Consistently, deletion of TRPP3NT abolished the off-response channel activity of the TRPP3-PKD1L3 complex expressed in HEK cells (34). To determine which domain(s)/residue(s) in TRPP3NT is critical for its channel function, we first generated several truncation mutants, named ⌬1-20 (with fragment Met-1-Trp-20 deleted), ⌬1-41, ⌬1-60, ⌬1-81, and ⌬1-95 (Fig. 1A). When expressed in oocytes, ⌬1-20 exhibited similar radiotracer Ca 2ϩ transport activity as the wild-type (WT) TRPP3, although the other mutants did not exhibit significant activity (Fig. 1B). Consistently, when the whole-cell currents were measured at Ϫ50 mV using the TEVC technique, ⌬1-20 and WT channels had similar channel function, although the other mutants did not produce any appreciable currents (Fig. 1, C and D). Similar results were obtained when currents were measured at other membrane potentials using a ramp protocol (Fig. 1E). We then performed immunofluorescence assays to examine the surface membrane localization of these mutants and found that these mutations do not significantly affect the surface membrane targeting (Fig. 1F). Taken together, these data demonstrate that the Asp-21-Ser-41 fragment is important for TRPP3 channel function.
We next performed further mutations truncating at various positions within Asp-21-Ser-41 and found that the function of ⌬1-30 and ⌬1-36 is similar to the WT channel, whereas mutants ⌬1-38 and ⌬1-40 completely lose their function with unaffected surface membrane localization (Fig. 2, A and B), indicating that residue Val-37 or Cys-38 is important for TRPP3 channel function. We then generated single point mutants V37A, C38A, and double point mutant V37A/C38A and found that only the C38A and V37A/C38A mutations result in substantially reduced channel activity, although the V37A mutation has little effect on channel activity (Fig. 2, C-E). Biotinylation assays showed that the surface membrane localization is not significantly affected by any of these mutations (Fig. 2F). Altogether, these data demonstrate that Cys-38, but not Val-37, is important for TRPP3 channel function.
Palmitoylation of TRPP3 at Cys-38 -We next examined the functional role of the other cysteine residues located outside the putative intra-membrane helices, including Cys-69, Cys-70, Cys-74, Cys-210, Cys-223, and Cys-512 (Fig. 3A). Mutations of these cysteine residues to alanine did not affect channel function (Fig. 3B). Thus, Cys-38, highly conserved among various species (Fig. 3C), is the only functionally important cysteine residue outside the putative membrane helices. Of note, based on sequence alignment, TRPP3 Cys-512 and its counterpart in human TRPP2 Cys-631 are both located within the short helix of their TM5-TM6 pore loop. Interestingly, TRPP2 Cys-631 was previously reported to be involved in disulfide bond formation and to be essential for its tetrameric assembly and channel function in HEK cells (35). Because of the presence of reducing cytosolic environments, it is unlikely that Cys-38 forms a disulfide bond with another cysteine residue from the same or a different TRPP3 monomer subunit. We thus wondered how Cys-38 contributes to TRPP3 channel function.
Recently, more and more ion channel proteins, such as the large conductance voltage-gated potassium channel and TRPML1, have been reported to be post-translationally modified by palmitoylation at cysteine residues to regulate channel trafficking and/or function (31)(32)(33). We then investigated whether TRPP3 Cys-38 is a palmitoylation site. First, we used palmitoylation prediction program CSS-Palm version 4.0 and found that Cys-38 has the highest palmitoylation score com-pared with the other N-terminal cysteine residues, Cys-69, Cys-70, and Cys-74 (Fig. 3D). We then treated TRPP3-expressing oocytes with widely used palmitoylation inhibitor 2-bromopalmitate (2BP) (31) overnight at various concentrations from 1 to 50 M, according to a previous report (36). TRPP3 channel currents measured at Ϫ50 mV and other membrane potentials were indeed reduced by 2BP in a dose-dependent manner (Fig.  4, A-C). Because immunofluorescence assays found that 2BP treatment has no effect on the TRPP3 plasma membrane expression (Fig. 4D), our data showed that 2BP treatment results in an inhibition of TRPP3 channel function in oocytes.
To verify the specificity of the 2BP effect on TRPP3 channel function, we wondered whether the inhibitory effect of 2BP on TRPP3 channel function can be competitively rescued by palmitic acid (PA), the natural substrate of the palmitoylation catalyzed by DHHC enzymes. For this, we treated TRPP3-expressing oocytes overnight with increasing concentrations of PA, from 0 to 20 M, in the presence of 20 M 2BP, which inhibited 80% of TRPP3 channel activity (Fig. 4B). Indeed, the inhibition of TRPP3 channel activity (measured at Ϫ50 mV or other membrane potentials) by 2BP was rescued by PA in a dose-dependent manner (Fig. 5, A-C). Again, we confirmed that TRPP3  45 Ca uptake in X. laevis oocytes expressing TRPP3 wild-type (WT) or mutants at day 3 following RNA injection. Oocytes injected with H 2 O were used as a negative control. Data were averaged from three independent experiments. *** indicates p Ͻ 0.001. C, representative whole-cell current traces obtained from Xenopus oocytes expressing TRPP3 WT or an indicated truncation mutant, using TEVC. Oocytes were voltage clamped at Ϫ50 mV. Data from H 2 O-injected oocytes served as a negative control. Currents were measured using the standard Na ϩ -containing extracellular solution without (STD) or with (STDϩCa) 5 mM CaCl 2 . D, averaged Ca 2ϩ -activated currents obtained at Ϫ50 mV from oocytes expressing TRPP3 WT or an indicated mutant or those injected with H 2 O. Currents were averaged from three independent experiments with total numbers of tested oocytes, as indicated. *** indicates p Ͻ 0.001. E, representative current-voltage relationship curves obtained using a voltage ramp protocol, as indicated, before (STD) and after (STDϩCa) addition of 5 mM CaCl 2 at the time point marked with a and b, respectively, in C. F, representative immunofluorescence data using oocyte slices, showing expression of TRPP3 WT and indicated truncation mutants.
surface membrane localization is not affected by these treatments, as shown by immunofluorescence data in oocytes (Fig.  5D). Thus, our rescue experiments using PA supported a specific effect of 2BP on TRPP3 channel function. We also treated TRPP3-expressing oocytes overnight with PA alone, from 1 to 20 M, but we found no effect on TRPP3 channel activity (Fig.  5E), which suggests that there may be a saturated amount of endogenous PA or its equivalent in oocytes. Taken together, these data strongly indicated that TRPP3 is modified by palmi-toylation, which is important for TRPP3 channel function, but not trafficking, in Xenopus oocytes.
We next wanted to provide further documents on the TRPP3 Cys-38 palmitoylation. It is known that palmitoylation of a transmembrane domain containing protein allows its cytosolic domains to anchor to the plasma membrane (37). We thus examined whether Cys-38 confers palmitoylation and attachment of the N-terminal domain of TRPP3 to the plasma membrane. For this, we overexpressed the EGFP-fused human  Fig. 1C. D, averaged Ca 2ϩ -activated currents obtained at Ϫ50 mV from oocytes expressing TRPP3 WT, V37A, C38A, or V37A/C38A. Currents were averaged from three independent experiments with indicated total numbers of tested oocytes. ** and *** indicate p Ͻ 0.01 and 0.001, respectively. E, representative current-voltage relationship curves obtained using a voltage ramp protocol, as indicated in Fig. 1E, before (STD) and after (STDϩCa) addition of 5 mM CaCl 2 . F, left panel, representative data on the plasma membrane (PM) expression of TRPP3 by biotinylation. Na ϩ /K ϩ -ATPase (PM marker) and ␤-actin (non-PM markers) were used as controls. Center and right panels, flow-through and total input data, respectively, from the same experiment.
TRPP3 N terminus, Met-1-Leu-95 (EGFP-TRPP3NT) in HEK cells, and detected EGFP epifluorescence to determine TRPP3NT cellular localization using confocal microscopy. We found that EGFP-TRPP3NT indeed shows plasma membrane expression, whereas EGFP-TRPP3CT (a TRPP3 C-terminal fragment, Glu-706 -Ser-805, as a negative control) exhibits intracellular distribution only (Fig. 6A). As expected, EGFP-N-Ras (a positive control), a well known palmitoylated oncoprotein, also attached to the plasma membrane in our experimental condition (Fig. 6A), consistent with its previously reported plasma membrane localization in COS-7 cells (38). To determine whether the plasma membrane expression of EGFP-TRPP3NT is due to palmitoylation, we attempted to disrupt palmitoylation by starving HEK cells in a fatty acid-free medium or treating cells with the palmitoylation inhibitor 2BP (100 M) overnight, as reported previously (38). Under both conditions, EGFP-TRPP3NT was found to stay in the cytoplasm (Fig. 6B), indicating that palmitoylation is required for the plasma membrane targeting of TRPP3NT. Similar results were also obtained for EGFP-N-Ras (Fig. 6B), which is consistent with the previous report using COS-7 cells (38). Furthermore, C38A mutation also resulted in localization of EGFP-TRPP3NT in the cytoplasm (Fig. 6B).
We next performed acyl-biotin exchange assays to directly determine whether TRPP3 is palmitoylated. For this, we transiently transfected FLAG-tagged TRPP3 WT and mutants FIGURE 3. Characterization of the TRPP3 other intracellular or extracellular cysteine residues and prediction of candidate palmitoylation residues. A, schematic illustration of all intracellular or extracellular cysteine residues in human TRPP3. B, averaged Ca 2ϩ -activated currents obtained at Ϫ50 mV from oocytes expressing TRPP3 WT or an indicated mutant. Currents were averaged from three independent experiments with indicated total numbers of tested oocytes. ** indicates p Ͻ 0.01. C, amino acid sequence alignment of TRPP3 N-terminal fragments containing Cys-38 or the corresponding cysteine from indicated species. National Center for Biotechnology Information accession number for sequences used here are as follows: NP_057196 (human); NP_852087 (mouse); NP_001099822 (rat); XP_001168415 (monkey); XP_012999134 (pig); XP_002718661 (rabbit); XP_006938169 (cat); and XP_005637930 (dog). Potential phosphorylation sites near the cysteine residue are marked with •. D, palmitoylation scores for cysteine residues in the human TRPP3 N terminus predicted by a CSS-palm version 4.0 algorithm. A higher score value indicates a higher probability.
C38A and T39E in HEK cells. TRPP3 was first immunoprecipitated with a rabbit anti-FLAG antibody and protein G-coated Sepharose beads. Immunoprecipitated TRPP3 proteins were then treated either with hydroxylamine to remove palmitate or with Tris base as a negative control. The exposed cysteine thiol groups were labeled with a thiol-reactive biotinylation reagent, 1-biotinamide-4[4Ј(maleimidomethyl)cyclohexane-carboxamido] butane (biotin-BMCC). The streptavidin-HRP antibody was then used to detect the palmitoylated TRPP3 and a mouse anti-FLAG antibody to detect total immunoprecipitated TRPP3. We indeed found that TRPP3 and mutant T39E, but not mutant C38A, are modified by palmitoylation (Fig. 6C). Furthermore, the TRPP3 palmitoylation was abolished by 2BP treatment overnight at a concentration of 100 M (Fig. 6C). These data together demonstrated that TRPP3 is indeed palmitoylated at Cys-38, which accounts for our observation that the plasma membrane targeting of TRPP3NT requires palmitoylation at Cys-38. Interestingly, the N terminus of TRPP2 (EGFP-TRPP2NT, Met-1-Lys-215) that possesses four cysteine residues also targeted to the plasma membrane when overexpressed in HEK cells, although the C terminus of TRPP2 (EGFP-TRPP2CT, Asp-682-Val-968) showed a cytosolic distribution (Fig. 6D), suggesting that the N-terminal palmitoylation is a shared mechanism by TRPP3 and TRPP2.
Phosphorylation of TRPP3 at Thr-39 -Because there have been reports about an interplay between palmitoylation and phosphorylation at a nearby site (37,39,40), we next examined potential phosphorylation sites near Cys-38. Five candidate phosphorylation sites, Thr-34, Thr-39, Ser-41, Ser-42, and Thr-43 are predicted in human TRPP3 by GPS 3.0 program (Fig. 3C). First, mutating any of these five sites to alanine did not affect channel function (41), suggesting either that these sites are not important or that expressed TRPP3 channels on the surface membrane are predominantly de-phosphorylated at one of these sites in Xenopus oocytes. We then mutated each of them to Glu to mimic phosphorylation and found that only mutation T39E significantly affects (substantially reduces) the channel function, although no mutation significantly alters the surface membrane localization (Fig. 7, A and B). Together with our observation that mutant T39D, compared with T39E, exhibited similarly impaired channel function and similar surface membrane localization (Fig. 7, A and B), our data suggest that Thr-39 is a functionally important phosphorylation site,  which is consistent with the fact that Thr-39 is conserved among different species (Fig. 3C).
We next further examined Thr-39 phosphorylation by Western blotting using human TRPP3NT with an N-terminal HA tag. When HA-TRPP3NT was transiently expressed in HEK cells, double bands were observed (Fig. 7C, left panel). The upper band disappeared following treatment by -phosphatase (PP) (Fig. 7C, left panel), which removes all phosphate groups from serine, threonine, and tyrosine residues. As a positive control, we found that human TRPP2NT, previously reported to be phosphorylated at Ser-76 (23), also displays double bands under our experimental conditions and that the upper band disappears by the PP treatment (Fig. 7C, right panel). Furthermore, mutation of Thr-39 to Ala, but not Ser-41 to Ala, eliminated the upper band of TRPP3NT (Fig. 7D). Taken together, our data indicate that TRPP3 is phosphorylated at the N-terminal Thr-39.
Relationship between Palmitoylation at Cys-38 and Phosphorylation at Thr-39 -We next investigated whether there is a correlation between palmitoylation at Cys-38 and phosphorylation at Thr-39 of TRPP3, given the presence of an interplay between these two types of post-translational modifications in some membrane proteins (31,39,40,42). For this, we examined whether the C38A mutation or Cys-38 de-palmitoylation reduces TRPP3 channel activity through increasing phosphorylation at Thr-39. First, introduction of the C38A mutation to the WT and T39A mutant channels resulted in similar reduction of channel activity (Fig. 8A). Second, treatment of oocytes expressing mutant T39A or WT TRPP3 with 20 M 2BP resulted in similar reduction of channel activity (Fig. 8A). As these mutations and 2BP treatments did not significantly affect surface membrane expression (Fig. 8B), we concluded that reduction of TRPP3 channel activity by de-palmitoylation is not through increasing phosphorylation at Thr-39. This conclusion was supported by our observation that C38A has little effect on the upper band of TRPP3NT (Fig. 8C).
Conversely, we examined whether the T39E mutation, which mimics phosphorylation at Thr-39, reduces TRPP3 channel activity through decreasing palmitoylation at Cys-38. Introduction of the T39E mutation to C38A mutant that cannot be palmitoylated further significantly reduced TRPP3 channel activity (Fig. 8D) without affecting plasma membrane expression (Fig. 8B), indicating that inhibition of TRPP3 channel function by phosphorylation at Thr-39 is not through decreasing palmitoylation at Cys-38. Furthermore, the T39E mutation had little effect on the plasma membrane localization of TRPP3NT (Fig. 8E) and palmitoylation of fulllength TRPP3 at Cys-38 (Fig. 6C). Taken together, these data showed that TRPP3 channel activity is regulated by palmitoy-

Discussion
So far, not much is known about TRPP3 post-translational modifications, although its homologue TRPP2 was reported to undergo phosphorylation, glycosylation, and disulfide bond formation (22,24,35). In this study, we found that TRPP3 is modified by palmitoylation and phosphorylation at the N-terminal cysteine 38 and threonine 39, respectively, and showed that these two post-translational modifications independently regulate TRPP3 channel function.
Palmitoylation is a dynamic post-translational modification that was first described 35 years ago in a transmembrane glycoprotein of vesicular stomatitis virus (43). 8 years later, in 1987, the first palmitoylated ion channel, rodent voltage-gated Na ϩ channel, was characterized (44). Since then, more than 50 different ion channels have been experimentally demonstrated to be palmitoylated (31). Increasing evidence has so far indicated that palmitoylation may regulate either the channel's membrane density or single channel activity (31). In the case of TRPP3, palmitoylation at Cys-38 had little effect on its plasma membrane expression, at least in Xenopus oocytes (Fig. 2F), but it dramatically reduced the channel activity (Fig. 2D) by a to-beidentified mechanism that is independent of phosphorylation at Thr-39. A surprising characteristic of TRP channels is that they can be activated by a wide variety of environmental stimuli. A shared mechanism underlying gating of TRPs by seemingly disparate activators was recently proposed by Liu and Montell (45) based on the discovery that a phospholipase C-dependent signaling cascade activates TRP channels in Drosophila photoreceptor cells through generation of force in the lipid bilayer. According to this theory, besides known mechano-sensitive TRP channels, other TRPs are also activated through mechanical forces formed by architectural changes in the cell membrane in response to different stimuli (45). TRPP2 was known to be co-localized with PKD1 in primary cilia of kidney cells where it is believed to act as part of a mechanical sensor (46). In con- trast, TRPP3 was reported to be co-localized with PKD1L1 in cilia (20) even though it remains unclear as to whether it is mechano-sensitive. It is generally assumed that palmitoylation facilitates the association of the protein to the membrane. Therefore, it is possible that TRPP3 palmitoylation has an interplay with the mechanical force exercised on the cell membrane with respect to channel gating. Alternatively, it remains to be determined whether palmitoylation regulates TRPP3 channel activity through facilitating an intramolecular interaction between its N-terminal pre-S1 and C-terminal TRP domains. This type of interaction was suggested to occur in TRPV1, TRPV2, TRPA1, and TRPV6 based on structural information revealed using cryo-EM or crystallography (3)(4)(5)(6).
TRPP3 is expressed in the brain (14), and a recent study using TRPP3 knock-out mice found that disruption of TRPP3 causes hippocampal and thalamocortical hyperexcitability and increases susceptibility to pentylenetetrazol-induced seizures (47). Interestingly, several neural proteins, including various G-protein-coupled receptors and ion channels that control the excitability of neurons, have now been reported to be dynamically regulated by palmitoylation (48). It would be interesting to see whether palmitoylation of TRPP3 at Cys-38 represents a mechanism underlying the control of TRPP3 channel activity in neurons with respect to neuronal excitability. TRPP3 was also found to interact with ␤2-adrenoreceptor (␤2AR) and co-localize with ␤2AR in the brain (47). Binding of agonist isoproterenol to ␤2AR was reported to markedly reduce the palmitoylation of the associated G␣ s (49). Thus, it is possible that ␤2AR regulates TRPP3 palmitoylation through physical binding. Furthermore, ␤2AR itself is also palmitoylated, and agonist-stimulated de-palmitoylation of ␤2AR was reported to promote its phosphorylation and ␤-arrestin-mediated receptor internalization (28). Therefore, it would be interesting to see whether there is an interplay between TRPP3 palmitoylation and ␤2AR, how this interplay is regulated, and whether it is involved in the control of neuronal excitability.
Post-translational modifications of TRP channels, such as glycosylation, phosphorylation, and covalent/reversible bind-  DECEMBER 2, 2016 • VOLUME 291 • NUMBER 49 ing of an activator to a cysteine residue, mainly affect their subcellular trafficking or channel activity (50). To date, within the TRP superfamily only, TRPML1 is known to be palmitoylated, both in a heterologous expression system and native stomach tissue, for regulation of its endocytosis (32,33). Thus, TRPP3 represents the first TRP member whose channel function is regulated by palmitoylation. It would thus be important to examine whether the function of other TRPs is also regulated by palmitoylation and to investigate the physiological implications of this type of post-translational modification. Palmitoylation is mostly mediated by a family of 23 (human) DHHC motif-containing palmitoyltransferases with unclear substrate specificities (37). De-palmitoylation, however, is mediated by acylprotein thioesterases (APTs), including APT1, APT2, and APT-like (37). Future studies would have to determine which DHHC enzyme(s) and acylprotein thioesterases are involved in TRPP3 palmitoylation and de-palmitoylation.

Palmitoylation Regulates TRPP3 Function
Phosphorylation at the C-terminal Ser-812 of TRPP2 by casein kinase II regulates its channel function, whereas phosphorylation at the N-terminal Ser-76 by glycogen synthase kinase 3 regulates its subcellular localization (22,23). Although phosphorylation of TRPP3 at the N-terminal Thr-39 abolishes its channel function, we still do not know which kinase is involved. Prediction by GPS 3.0 program suggests that a PKC kinase phosphorylates TRPP3 at Thr-39. Of note, the fact that mutant T39A displayed a similar functional activity as the WT channel suggests that TRPP3 channels in oocytes are mostly de-phosphorylated, which is consistent with our data obtained from Western blotting experiments (Fig. 7D). It is also interesting to determine whether TRPP3 is phosphorylated at other sites and, if any, what are the corresponding functional roles. Furthermore, although palmitoylation at Cys-38 and phosphorylation at Thr-39, the only phosphorylation site proximate to Cys-38, are both functionally important for TRPP3, our experiments showed that they are not linked to each other. This is in contrast to previously reported ion channels with respect to an interplay between the two modifications. For example, large conductance Ca 2ϩ -and voltage-gated K ϩ channels were found to be inhibited by PKA phosphorylation of a C-terminal serine residue, immediately upstream of a conserved palmitoylated cysteine residue, by reducing palmitoylation to disrupt the anchorage of their C terminus to the plasma membrane (39). Thus, it could be that TRPP3 palmitoylation at Cys-38 is not linked to any phosphorylation or to a phosphorylation that is not close to Cys-38, which would suggest that TRPP3 palmitoylation may represent a novel and yet-to-be determined way of functional regulation. Because both phosphorylation and palmitoylation are of dynamic and reversible regulation mechanisms, it would be important to elucidate how the function of other TRPs is regulated by the two modifications and to examine potential cross-talk between them.
In summary, this study has identified N-terminal Cys-38 as a palmitoylation site that mediates anchorage of the N terminus to the surface membrane and regulates TRPP3 channel function. We have also identified N-terminal Thr-39 as a phosphorylation site critical for TRPP3 channel function. Furthermore, we have shown that the palmitoylation and phosphorylation independently regulate TRPP3 channel function, which we think may represent a novel mechanism of regulation that deserves further studies.

Experimental Procedures
Vectors, Plasmids, and Antibodies-Human full-length TRPP3 cDNA was subcloned into vector pCHGF (41) for X. laevis oocyte expression. FLAG tag was then inserted 5Ј of the TRPP3 coding region for detection. cDNAs coding for the N or C termini of human TRPP3 and TRPP2 were subcloned into the pEGFPC2 vector for mammalian cell expression. All mutations were made with QuikChange Lightning Site-directed Mutagenesis kit (Agilent Technologies, La Jolla, CA) and confirmed by sequencing. Rabbit antibodies against FLAG (D-8), Na ϩ /K ϩ -ATPase (H-300), and mouse antibodies against ␤-actin (C-4) were purchased from Santa Cruz Biotechnology (Santa Cruz, CA). Mouse antibody against HA (HA.C5) was purchased from Abcam (Cambridge, MA). Secondary antibodies were purchased from GE Healthcare.
Preparation of mRNAs and Microinjection into Oocytes-pCHGF plasmids containing TRPP3 WT or mutant cDNAs were linearized with MluI, followed by phenol/chloroform purification and ethanol precipitation. Linearized DNAs were then used to in vitro synthesize capped mRNAs using mMES-SAGE mMACHINE kit (Ambion, Austin, TX). Stage V-VI oocytes were isolated from X. laevis. Defolliculation of oocytes was performed through incubation in Ca 2ϩ -free Barth's solution (51) containing collagenase (2 mg/ml) at room temperature for 1 h. Oocytes were then incubated at 18°C in the Barth's solution for at least 3 h before injection of 25 nl of RNase-free water containing 25 ng of mRNAs using picospritzer III (Parker Hannifin, Cleveland, OH). An equal volume of water was injected into each control oocyte. This study was approved by the Ethical Committee for Animal Experiments of the University of Alberta and was carried out in accordance with the Guidelines for Research with Experimental Animals of the University of Alberta and the Guide for the Care and Use of Laboratory Animals (National Institutes of Health Guide) revised in 1996. Injected oocytes were incubated at 18°C in the Barth's solution supplemented with antibiotics for 2-4 days prior to experiments. 45 Ca Uptake-Radiotracer uptake experiments were performed as described previously (15). In brief, radioactive 45 CaCl 2 (Amersham Biosciences, UK) at 30 M was added to the uptake solution (100 mM N-methyl-D-glucamine, 2 mM KCl, 1 mM MgCl 2 , 10 mM HEPES, pH 7.5) plus 1 mM non-radioactive CaCl 2 . Ten oocytes of each sample were incubated in 0.5 ml of the uptake solution for 30 min, and the incubation was terminated by washing oocytes with ice-cold NaCl-containing solution (100 mM NaCl, 2 mM KCl, 1 mM MgCl 2 , 10 mM HEPES, pH 7.5). Individual oocytes were then dissolved in 250 l of 10% SDS and mixed with 2.5 ml of scintillation mixture prior to scintillation counting.
Two-electrode Voltage Clamp-TEVC experiments were performed as described before (41). Briefly, the two electrodes (capillary pipettes, Warner Instruments, Hamden, CT) impaling an oocyte were filled with 3 M KCl to form a tip resistance of 0.3-2 megohms. The standard extracellular solution containing 100 mM NaCl, 2 mM KCl, 1 mM MgCl 2 , and 10 mM HEPES, pH 7.5, with or without 5 mM CaCl 2 was used. The duration of application of Ca 2ϩ solution was indicated in time course recordings. The palmitoylation inhibitor 2BP (Sigma) was made as a fresh 100 mM stock in DMSO and applied at various concentrations from 1 to 50 M overnight. Oocyte whole-cell currents were recorded using a Geneclamp 500B amplifier and Digidata 1322A AD/DA converter (Molecular Devices, Union City, CA). The pClamp 9 software (Axon Instruments, Union City, CA) was employed for data acquisition and analysis. Currents and voltages were digitally recorded at 200 s/sample and filtered at 2 kHz through a Bessel filter. SigmaPlot 12 (Systat Software, San Jose, CA) was used for data fitting and plotting.
Oocyte Immunofluorescence-Immunofluorescence assays using oocyte slices were performed as described previously (41). Whole-mount staining was performed as follows: Xenopus oocytes were washed in PBS, fixed in 4% paraformaldehyde for 15 min, washed three times in PBS plus 50 mM NH 4 Cl, and then permeabilized with 0.1% Triton X-100 for 4 min. Oocytes were then blocked in PBS plus 3% skim milk for 30 min, and then incubated overnight with the rabbit anti-TRPP3 polyclonal antibody (catalog no. PAB5914, Abnova, Taiwan), followed by incubation with a secondary AlexaFluor 488-conjugated donkey anti-rabbit antibody (Jackson ImmunoResearch, West Grove, PA) for 30 min. Oocytes were then mounted in Vectashield (Vector Labs, Burlington, Ontario, Canada) and examined on an AIVI spinning disc confocal microscopy (Cell Imaging Facility, Faculty of Medicine and Dentistry, University of Alberta).
Western Blotting-Protein samples were prepared with Cel-Lytic M lysis buffer (Sigma) from oocytes or mammalian cells according to the manufacturer's instruction. 50 -80 g of total proteins were then separated on 8% SDS-polyacrylamide gels and transferred to nitrocellulose membranes that were then blocked for 1 h at room temperature with 3% skim milk in PBS buffer supplemented with 1% Tween 20. This was followed by overnight incubation at 4°C with diluted primary antibodies in blocking buffer according to suppliers' suggestions. Secondary horseradish peroxidase-coupled anti-mouse and anti-rabbit antibodies were purchased from GE Healthcare.
Biotinylation-Xenopus oocytes were washed three times with PBS followed by incubation with 0.5 mg/ml sulfo-NHS-SS-Biotin (Pierce) for 30 min at room temperature. 1 M NH 4 Cl was used to quench the non-reacted biotin. Oocytes were then washed with PBS and harvested in ice-cold CelLytic TM M lysis buffer (Sigma) supplemented with proteinase inhibitor mixture (Thermo Scientific, Waltham, MA). Lysates were incubated at room temperature for 3 h with gentle shaking upon addition of 100 l of streptavidin (Pierce). The surface protein absorbed by streptavidin was resuspended in SDS and subjected to SDS-PAGE.
Mammalian Cell Culture, Transfection, and Treatments-HEK293 cells were cultured in Dulbecco's modified Eagle's medium (DMEM) supplemented with 10% fetal bovine serum (FBS) and 1% penicillin/streptomycin (Sigma). Transient transfection was performed using Lipofectamine 2000 (Invitrogen) according to the manufacturer's instruction. The palmitoylation inhibitor 2-BP (Sigma) was made as a fresh 100 mM stock in DMSO and applied at a final concentration of 100 M over-night. For fatty acid starvation, cells were incubated overnight with DMEM supplemented with 10% FBS treated with 5% dextran-coated charcoal (Sigma).
Confocal Imaging-Transfected HEK cells were washed in PBS and fixed in 4% paraformaldehyde for 15 min followed by permeabilization in 0.1% Triton X-100 for 15 min at room temperature. Cells were then blocked with 3% bovine serum albumin in PBS for 30 min. Where indicated, cells were stained with mouse antibody against Na ϩ /K ϩ -ATPase (catalog no. ab7671, Abcam) or rat 1:200 dilution for 1 h at room temperature, followed by incubation with a secondary Cy3-conjugated goat anti-mouse antibody (Jackson ImmunoResearch) for 30 min. Cells were then mounted in ProLong Diamond Antifade Mountant with DAPI (Molecular Probes, Eugene, OR) and examined on an AIVI spinning disc confocal microscopy (University of Alberta).
Acyl-Biotin Exchange Assay-Transfected or treated HEK cells were washed three times in PBS and lysed in 500 l of lysis buffer (LB, 1% IGEPAL CA-630, 50 mM Tris-HCl, pH 7.5, 150 mM NaCl, and 10% glycerol) supplemented with protease inhibitor mixture (Thermo Scientific) and 50 mM freshly made N-ethylmaleimide (Thermo Scientific). Acyl-biotin exchange experiments were performed as described previously (52). In brief, proteins were immunoprecipitated with rabbit anti-FLAG antibody (catalog no. ab1162, Abcam) and 50% slurry of protein G-coated Sepharose beads (GE Healthcare). After washing three times with LB supplemented with 0.1% SDS, each sample of beads was split into two with one incubated with 500 l of LB, pH 7.2, and the other with the same volume of LB containing 1 M hydroxylamine (Sigma) to cleave the thioester bond. The samples were rotated at room temperature for 1 h. After the beads were washed once in LB, pH 6.2, the samples were incubated with 3 M biotin-BMCC (Thermo Scientific) in LB, pH 6.2, to label the unmasked free thiol groups of cysteine residues. The biotin-conjugated proteins were then eluted with 2ϫ SDS loading buffer, subjected to SDS-PAGE, and blotted with streptavidin-HRP antibody (Thermo Scientific) or mouse anti-FLAG antibody (catalog no. 8146, Cell Signaling Technology, Danvers, MA).
Statistical Analysis-Data were analyzed and plotted using SigmaPlot 12 (Systat Software) and expressed as means Ϯ S.D., where S.D. is standard deviation. One-way analysis of variance with a post-hoc test (Bonferroni adjustment) was used to compare two sets of data. A probability value (p) of less than 0.05, 0.01, and 0.001 was considered statistically significant and indicated by *, **, and ***, respectively.