H. Kahr and R. Schindl contributed equally to the work.
CaT1 knock-down strategies fail to affect CRAC channels in mucosal-type mast cells
Article first published online: 4 MAY 2004
The Journal of Physiology
Volume 557, Issue 1, pages 121–132, May 2004
How to Cite
Kahr, H., Schindl, R., Fritsch, R., Heinze, B., Hofbauer, M., Hack, M. E., Mörtelmaier, M. A., Groschner, K., Peng, J.-B., Takanaga, H., Hediger, M. A. and Romanin, C. (2004), CaT1 knock-down strategies fail to affect CRAC channels in mucosal-type mast cells. The Journal of Physiology, 557: 121–132. doi: 10.1113/jphysiol.2004.062653
- Issue published online: 4 MAY 2004
- Article first published online: 4 MAY 2004
- (Resubmitted 11 February 2004; accepted after revision 11 March 2004; first published online 12 March 2004)
CaT1, the calcium transport protein 1 encoded by TRPV6, is able to generate a Ca2+ conductance similar but not identical to the classical CRAC current in mucosal-type mast cells. Here we show that CaT1-derived Ca2+ entry into HEK293 cells is effectively inhibited either by expression of various dominant negative N-terminal fragments of CaT1 (N334-CaT1, N198-CaT1 and N154-CaT1) or by antisense suppression. By contrast, the endogenous CRAC current of the mast cells was unaffected by CaT1 antisense and siRNA knockdown but markedly suppressed by two (N334-CaT1, N198-CaT1) of the dominant negative N-CaT1 fragments. Inhibition of CRAC current was not an unspecific, toxic effect, as inward rectifier K+ and MagNuM currents of the mast cells were not significantly affected by these N-CaT1 fragments. The shortest N154-CaT1 fragment inhibited CaT1-derived currents in mast cells, but failed to inhibit CRAC currents. Thus, the structural requirements of rCaT N-terminal fragments for inhibition of rCaT1 and CRAC channels are different. These results together with the lack of CaT1 antisense and siRNA effects on currents render it unlikely that CaT1 is a component of native CRAC channels in mast cells. The data further demonstrate a novel strategy for CRAC current inhibition by an N-terminal structure of CaT1.
In non-excitable cells generation of inositol trisphosphate (IP3) by stimulation of phospholipase C subtypes leads to a rapid release of Ca2+ from the endoplasmic reticulum store, which is followed by a slow and sustained entry of extracellular Ca2+ through store-operated channels (Bootman et al. 2001; Putney et al. 2001; Venkatachalam et al. 2002). A highly calcium-selective store-operated current, termed calcium release activated calcium (CRAC) current (Parekh & Penner, 1997; Lewis, 1999), has been found in mast cells and T-lymphocytes.
Molecular candidates for mammalian store-operated calcium channels are found within the transient receptor potential (TRP) superfamily (Harteneck et al. 2000; Clapham et al. 2001; Montell, 2001; Gunthorpe et al. 2002; Montell et al. 2002; Zitt et al. 2002) that consists of the TRPC, TRPV and TRPM subgroups. Among these, the calcium transport protein 1 (CaT1) encoded by TRPV6 has been proposed to manifest pore properties of CRAC channels (Yue et al. 2001), particularly the high selectivity for Ca2+. Conflicting results are published, however, on the activation mechanism of CaT1. CaT1 has been found to generate either store-operated (Yue et al. 2001; Vanden Abeele et al. 2003), or constitutively active conductances (Voets et al. 2001; Bodding et al. 2002; Cui et al. 2002). We have demonstrated that a low level of CaT1 expression leads to store-operated CaT1 currents in mucosal-type rat basophilic leukaemia (RBL) mast cells (line RBL-2H3), whereas high expression levels of CaT1 yield constitutively active currents (Schindl et al. 2002). Recently it has been reported (Cui et al. 2002) that a pore mutant of CaT1 suppresses CRAC current activation in T-lymphocytes. Beside this and other similarities of CaT1 and CRAC channels, clear differences have been found in the current–voltage relationship of CaT1 and CRAC currents in a divalent free extracellular medium (Schindl et al. 2002). Additionally, ion selectivity and unitary conductance of CaT1 and CRAC channels are different (Voets et al. 2001; Prakriya & Lewis, 2002). Nonetheless, these observations still leave the possibility of CaT1 being a subunit of CRAC channels.
In the present study we examined whether rat CaT1 (rCaT1) has a role in CRAC channels of RBL mast cells by an approach that combined RT-PCR, antisense, siRNA and dominant negative knockdown strategies. While the antisense and siRNA approach was effective in eliminating rCaT1-derived currents, CRAC activity was not altered in RBL cells. Among the three N-terminal fragments of rCaT1 that function as a dominant negative species, two of them suppressed rCaT1 activity and were also able to inhibit CRAC currents in mast cells. The shortest N-terminal fragment, however, failed to inhibit CRAC currents while its dominant negative effect on rCaT1 was still preserved. Hence, the structural requirements of rCaT N-terminal fragments for inhibition of rCaT1 and CRAC channels are different.
Cell culture and molecular cloning
Experiments were performed on a secreting subline (2H3) of RBL mast cells and HEK293 cells cultured according to (Schindl et al. 2002). Lymph node carcinoma of the prostate (LNCaP) human prostate cancer epithelial cell line (DSMZ, Germany) were grown in RPMI Medium 1640 supplemented with 10% fetal bovine serum, 2 mm glutamine and 2 U ml−1 penicillin and 2 mg ml−1 streptomycin, in a humidified atmosphere with 5% CO2 at 37°C.
The coding region of rCaT1 (accession no. AF160798) was cleaved from pTracer-CMV2 (Invitrogen, USA) and transferred to the plasmid pECFP-C1 or pEYFP-C1 (Clontech, Germany) resulting in the respective amino-terminal tagged clones. For the production of the 334 amino acid (aa), 198 aa and 154 aa N-terminal fragments, three interior restriction sites, BsaAI (334 aa), ScaI (198 aa) and StuI (154 aa) were selected. All constructs were subcloned in pTracer-CMV2 and termed N334-rCaT1, N198-rCaT1 and N154-rCaT1. To construct the antisense rCaT1, the complete coding cDNA of rCaT1 was subcloned in pcDNA3 (Invitrogen, USA) in antisense orientation. N302-TRPC3 was cloned from TRPC3 (accession no. U47050) as described (Groschner et al. 1998). The integrity of all the constructed clones was confirmed by restriction digests and sequence analysis (VBC Genomics, Austria).
The siRNAs were purchased (Dharmacon Research, USA) and had the following sequences: control siRNA: AAUCAUCUAAGCUGGCUUUGC; and CaT1-siRNA: AACCUGCUGCAGCAGAAGAGG. The latter sequence is fully conserved in both rat and human CaT1.
The isolated RNA was reverse transcribed using the SuperScript First-Strand Synthesis System (Invitrogen, USA). RNA was quantified using UV light spectrophotometry, and the integrity of the RNA was confirmed by gel electrophoresis. To relate the amount of CaT1 to GAPDH cDNA in the reverse-transcribed samples, real time PCR analysis was performed in the LightCycler System (Roche Molecular Biochemicals, USA) using the following conditions and primers. Each cycle consisted of denaturation for 20 s at 95°C, annealing for 5 s at 65°C (hCaT1), 56°C (rCaT1) or 60°C (human and rat GAPDH), and extension for 25 s at 72°C, with a temperature transition rate of 8°C s−1. Detection of SYBR green fluorescence was performed for 3 s at 86°C (hCaT1), 82°C (rCaT1) or 85°C (GAPDH); primer sequences used for PCR are as follows: hCaT1 forward 5′-AGCCTACATGACCCCTAAGGACG-3′, hCaT1 reverse 5′-GTAGAAGTGGCCTAGCTCCTCGG-3′; rCaT1 forward 5′-CCCGATGAGCTGGGCCATTTCT ATG-3′, rCaT1 reverse 5′-CAGAGTAGAGGTCATCTTGTTGCTG -3′; GAPDH forward 5′-TCACCATCTTCCAGGAGCG-3′, GAPDH reverse 5′-CTGCTTCACCACCTTCTTGA-3′.
RBL cells were transfected by electroporation with 20 μg of pTracerCMV2-rCaT1, 40 μg of pTracerCMV2-N-terminal rCaT1 fragments (with 334, 198 or 154 aa), pcDNA3-antisense-rCaT1 or 5.3 μg (200 nm) CaT1-siRNA. Transfection of HEK cells (Schindl et al. 2002) was performed using SuperFect (Qiagen, Germany) with 1 μg of pTracerCMV2-rCaT1 or CFP-/YFP-rCaT1, 2–5 μg antisense-rCaT1, 1.25 μg N334-rCaT1, 0.77 μg N198-rCaT1 or N154-rCaT1. Transfected cells were identified by green fluorescent protein (GFP) coexpression encoded in the pTracerCMV2 plasmid or directly via YFP-/CFP-tagged proteins. Specifically, quantification of the number of cells expressing YFP-rCaT1 was carried out by setting a threshold fluorescence intensity level (10% above the background of 60 counts) above which cells were counted as positively expressing cells. Measurements were carried out 24–72 h following electroporation or transfection. For transfection of LNCaP cells, 2 μl Lipofectamin 2000 together with 200 nm CaT1-siRNA or control siRNA was used. Positively tranfected LNCaP cells were identified by the expression of cotransfected GFP. Recordings were performed 72 h after transfection.
Electrophysiological experiments were performed (Schindl et al. 2002) at 20–24°C, using the patch-clamp technique (Hamill et al. 1981) in the whole-cell recording configuration. Voltage ramps were usually applied every 5 s from a holding potential of 0 mV or +70 mV, covering a range of −90 to +90 mV over 1 s or 200 ms. In RBL mast cells, activation of CRAC currents (observed in all RBL cells) was monitored applying the 1 s voltage ramp at a holding potential of 0 mV and leak-corrected currents were measured at −74 mV. In all recordings that were performed in divalent free (DVF) solutions, a 100 ms ramp (−90 mV to +90 mV) was applied every 2 s from a holding potential of 0 mV according to Voets et al. (2001). The pipette solution used to passively deplete intracellular Ca2+ stores contained (mm): 145 caesium methane sulphonate, 8 NaCl, 3.5 MgCl2, 10 Hepes, 10 EGTA, pH 7.2. For active store depletion, 20 μm IP3 and 4.3 mm CaCl2 to maintain 100 nm intracellular Ca2+ were added. MagNuM currents of RBL cells were measured without intracellular MgCl2. Pipette solution for inward rectifier currents was (mm): 145 KCl, 1 MgCl2, 10 glucose, 10 Hepes, pH 7.4 (KOH). Bath solution included 140 NaCl, 5 KCl, 1 MgCl2, 2 CaCl2, 10 glucose, 10 Hepes, pH 7.4 (NaOH). Extracellular solution usually consisted of (mm): 145 NaCl, 5 CsCl, 1 MgCl2, 10 Hepes, 10 glucose, 10 CaCl2, pH 7.4. Divalent free (DVF) solution consisted of (mm): 165 NaCl, 5 CsCl, 10 Hepes, 10 glucose, 10 EDTA, pH 7.4 (CsOH).
Fluorescence resonance energy transfer (FRET)
Tranfected HEK cells grown on coverslips for 1 day were transferred to an extracellular solution identical to the bath solution used to record inward rectifier currents (see above). A QLC100 Real-Time Confocal System (VisiTech Int., UK) was used for recording images and was connected to two Photometrics CoolSNAPHQ monochrome cameras (Roper Scientific, USA). This system was attached to an Axiovert 200M microscope (Zeiss, Germany) in conjunction with an argon ion multi-wavelength (457, 488, 514 nm) laser (Laser Physics Inc., USA). The wavelenghts were selected by an Acousto Optical Tuneable Filter (VisiTech Int., UK). The dual port adapter contains a 505lp dichroic, a 485/30 cyan emission filter and a 535/50 yellow emission filter (Chroma Technology Corp., USA). MetaMorph 5.0 software (Universal Imaging Corp.) was used to acquire images and to control the confocal system.
The FRET image has to be corrected due to a cross-talk from one channel to the other. For this, the corrected FRET image (nFRET) was calculated after background subtraction using a custom-made software integrated in MatLab 6 according to the following equation (Xia & Liu, 2001):
denotes the background corrected intensity of the FRET image (excitation 457 nm, emission 535 nm), IYFP the background corrected intensity of the YFP image (excitation 514 nm, emission 535 nm) and ICFP the background corrected intensity of the CFP image (excitation 457 nm, emission 485 nm). The CalCFP factor and the CalYFP factor were obtained from experiments where only CFP or YFP was expressed (CalYFP=IFRET/IYFP= 0.4; CalCFP=IFRET/ICFP= 0.4).
Ca2+ fluorescence measurements
RBL cells were grown on coverslips for 1 day and loaded with fura-2/AM (1 μm) for 20 min at 20°C in Dulbecco's modified Eagle's medium (see Cell culture and molecular cloning) and washed three times; dyes were allowed to deesterify for 15 min at 20°C. Coverslips were transferred to an extracellular solution without Ca2+ and mounted at an inverted Axiovert 100 TV microscope (Zeiss, Germany). Excitation of Fura-2 was performed at 340 nm and 380 nm, and Ca2+ measurements are shown as 340/380 ratios of both GFP and untransfected RBL cells.
Results are presented as means ±s.e.m. calculated for the indicated number of experiments. Student's two-tailed t test was used for statistical comparison considering differences statistically significant at P < 0.05.
rCaT1 has been proposed to manifest pore properties of CRAC channels, particularly due to its high selectivity for Ca2+ (Yue et al. 2001). A quantitative comparison of the levels of CaT1 mRNA expression in RBL and LNCaP cells yielded GAPDH-normalized values ((CaT1/GAPDH) × 103) of 0.000000 (below the detection limit) and 3.797823, respectively, confirming CaT1 expression in LNCaP (Peng et al. 2001; Wissenbach et al. 2001). The expression of endogenous rCaT1 in RBL mast cells may have also failed biochemical detection by Northern blot analysis (Bodding et al. 2002) probably due to extremely low mRNA levels, although the rCaT1 clone used in this study was derived from the RBL mast cells (Yue et al. 2001).
Hence, to ultimately evaluate a contribution of rCaT1 protein to CRAC activity in RBL mast cells, we alternatively employed antisense (AS) and siRNA knock-down strategies to inhibit rCaT1 protein expression. We initially started with an antisense (AS) approach to inhibit rCaT1 protein expression. The efficiency of the constructed rCaT1-antisense (rCaT1-AS) was assessed in HEK cells by a reduction in the expression of yellow fluorescent protein (YFP)-tagged rCaT1 (Fig. 1A) or in the level of rCaT1-derived currents (Fig. 1B and C). The amount of YFP-rCaT1 was significantly reduced by coexpression of rCaT1-AS (2-fold or 5-fold excess; Fig. 1A). Consistently, coexpression of rCaT1 and rCaT1-AS led to a significant reduction of the constitutively active rCaT1-derived currents in HEK cells substantiating the efficiency of our rCaT1-AS probe. Specificity of this probe was confirmed by a small yet not significant inhibition of human calcium transport protein 1 (hCaT1)-derived currents (Fig. 1D and E).
In RBL mast cells, expression of rCaT1 leads to the formation of store-operated rCaT1 channels that are activated similar to endogenous CRAC currents, resulting in an about twofold increase in current density (Schindl et al. 2002). When rCaT1-AS was coexpressed with rCaT1 cDNA in these mast cells, a reduction of Ca2+ inward current was observed to the current level usually reached by CRAC (Fig. 2A–D) indicating that endogenous CRAC currents remained unaffected. The complete suppression of rCaT1-derived currents by rCaT1-AS was substantiated by analysis of current–voltage relationships in divalent free solution (Voets et al. 2001; Schindl et al. 2002) that enabled clear differentiation between CRAC and rCat1 currents (Fig. 2D). The fingerprint of rCaT1 (Voets et al. 2001; Schindl et al. 2002) represented by a negative slope in the current–voltage relationship (arrow in Fig. 2D) was absent in CRAC currents from control RBL mast cells and was abolished in cells cotransfected with both rCaT1 and rCaT1-AS (Fig. 2D).
As an alternative second approach, siRNA against CaT1 was employed to knock-down potential endogenous CaT1 (Fig. 3). LNCaP cells that posses a store-operated Ca2+ channel partially involving CaT1 (Skryma et al. 2000; Vanden Abeele et al. 2003) were initially used to estimate optimal siRNA concentrations based on a reduction of 45Ca influx (data not shown). Then, effective concentrations of 200 nm siRNA were examined on depletion-activated endogenous CaT1 currents in LNCaP cells (Fig. 3A and B) resulting in a significant reduction of these Ca2+ currents when compared to the effect of control siRNA consistent with Vanden Abeele et al. (2003). However, the same siRNA failed to reduce CRAC currents in RBL mast cells (Fig. 3C and D), although the current derived from rCaT1 overexpressed in these cells was significantly reduced to the level of endogenous CRAC current (Fig. 3E and F). Consistently, efficacy of siRNA on overexpressed YFP-tagged rCaT1 in RBL cells was observed by both an about 2.3-fold reduction in cells exhibiting an average fluorescence intensity above background and an about 10-fold reduction in their average fluorescence intensity level when compared with control (data not shown). Thus, the lack of effect of CaT1 antisense and siRNA knockdown strategies on CRAC currents suggests that rCaT1 is not a component of the native CRAC current in RBL mast cells.
In a third approach we tested for an effect of dominant negative rCaT1 species on CRAC activity in RBL mast cells. Based on the finding that TRPV proteins yield a functional channel associated with their ability to form a tetrameric structure (Kedei et al. 2001; Hoenderop et al. 2003) via their amino (N)-terminus (Xu et al. 1997), we first confirmed in vivo assembly of rCaT1 proteins, and then later on examined the interaction capability of expressed N-terminal fragments of CaT1. Thus rCaT1 was labelled at the N-terminus with either cyan fluorescent protein (CFP) or yellow fluorescent protein (YFP), and both differentially labelled proteins were coexpressed at a 1: 1 molar ratio in HEK cells. Assembly of rCaT1 proteins was evaluated from fluorescence resonance energy transfer (FRET) measurements (Fig. 4). The corrected FRET image (Fig. 4A, upper panel d; nFRET, see Methods) depicts higher nFRET values for HEK cells expressing both CFP-rCaT1 and YFP-rCaT1 compared to control cells expressing CFP and YFP-rCaT1 (Fig. 4C). The statistical evaluation of average nFRET values indicated significantly higher nFRET when both rCaT1 proteins are labelled (Fig. 4C), in line with the formation of rCaT1 tetramers (Hoenderop et al. 2003). This tetramer formation might involve the N-terminus of rCaT1 as evident from FRET experiments with coexpressed CFP-/YFP-labelled N-termini of rCaT1 in HEK cells (Fig. 4B). As compared to control cells, significantly higher nFRET values were calculated when both N-termini (N198-rCaT1, see below) were labelled (Fig. 4B and D) pointing to an interacting capability inherent to the N-terminal portion of rCaT1.
Additional experiments were carried out to determine FRET between N198-rCaT1 and rCaT1 proteins labelled by CFP and YFP, respectively. Interestingly, we could not detect a significant (t test, P > 0.05) difference between control CFP + YFP-rCaT1 (n= 9) and CFP-N198-rCaT1 + YFP-rCaT1 (n= 11) nFRET average values when calculated from whole cell areas. To reveal a possible weak interaction between CFP-N198-rCaT1 and YFP-rCaT1, we performed another type of analysis based on the comparison of those nFRET values in these distributions which are lying above an upper limit that comprises 95% of nFRET values of the control distribution (CFP + YFP-rCaT1). Here we determined that the probability of detecting nFRET is about 110-fold and 70-fold higher with interacting N-terminal fragments and whole CaT1 proteins, respectively, than with N-terminal fragment + CaT1 proteins (data not shown). This weak and less frequently occurring interaction of N-terminal rCaT1 fragment with rCaT1 compared to that of N-terminal rCaT1 fragments is consistent with results from Montell's group (Xu et al. 2001) where a much stronger interaction has been reported for the N-terminal fragments of TRP-related protein (MLSN-S) in comparison to that of the N-terminal fragment (MLSN-S) with the whole TRP-related protein (MLSN-L).
Based on these findings and on previous reports (Xu et al. 1997; Groschner et al. 1998) that have demonstrated TRP protein interactions via the N-terminal strand, we tested for a potential dominant negative effect of the N-terminus of rCaT1 which might substitute for rCaT1 in a tetramer resulting in formation of non-functional rCaT1 channels. For this, we coexpressed the N-terminus of rCaT1 (N334-rCaT1) together with rCaT1 in HEK cells and compared their inward currents with those of control HEK cells expressing only rCaT1. The N334-rCaT1 significantly suppressed rCaT1-derived Ca2+ inward currents (Fig. 5A and B) thus representing a tool with an efficient dominant negative effect on CaT1-containing channels. Consistently, expression of a CaT1 mutant where the N-terminus was deleted failed to produce detectable currents, supporting its importance in the formation of functional channels (data not shown). To further narrow the domain within the N334-rCaT1, shorter N-termini of rCaT1 (N198-rCaT1, N154-rCaT1) were generated and were found to be similarly effective as the longer form in suppressing rCaT1-derived currents (Fig. 5C–F). These results localize the dominant negative domain of the N-terminus of rCaT1 within the first 154 amino acids. The mechanism(s) responsible for the dominant negative effect of N-terminal rCaT1 fragments will be the focus of further studies, as the interaction between whole rCaT1 and N198-rCaT1 based on FRET analysis as mentioned before seems to be weak despite the strong dominant negative effect. Consistently, a strong dominant negative effect was observed for the N-terminal fragment (MLSN-S) with the whole TRP-related protein (MLSN-L) despite a weak interaction (Xu et al. 2001). Four ankyrin-like repeats have been identified within the 198 amino acids (Peng et al. 1999) that might contribute to the observed dominant negative effect of the N198-rCaT1. To examine for a possible involvement of the ankyrin-like repeats, the N-terminus of TRPC3 (N302-TRPC3) exhibiting four such repeats was employed as a surrogate. Co-expression of N302-TRPC3 with rCaT1, however, did not significantly suppress rCaT1-derived currents (Fig. 5G and H). This finding renders it unlikely that ankyrin-like repeats are responsible for the observed dominant negative effect of the various N-terminal fragments and favours a role of these fragments in disturbing the formation of functional channels.
Thus having established the dominant negative effect of the N-terminal rCaT1 fragments on rCaT1-derived currents, we examined their effects on the endogenous CRAC currents in RBL mast cells. In contrast to the results of the rCaT1 antisense and siRNA experiments, expression of the N334-rCaT1 (data not shown) and N198-rCaT1 fragments substantially suppressed activation of endogenous CRAC (Fig. 6A–C). This suppression was observed when activation of CRAC currents was induced either by passive (10 mm EGTA; Fig. 6A–C) or active (20 μm IP3+100 nm Ca2+, data not shown, P < 0.05, n= 6) store depletion. Additionally, the store-operated Ca2+ current obtained by rCaT1 expression in RBL cells (Schindl et al. 2002) was similarly depressed by N198-rCaT1 (data not shown, P < 0.001, n= 6). To assess that the blocking effect of N198-rCaT1 is not an unspecific impairment of cell function, we tested its effect on the inward rectifier K+ (Wischmeyer et al. 1995) and MagNuM (Kozak et al. 2002) currents of RBL mast cells (Fig. 6G–J). Both currents were not significantly affected by N198-rCaT1. Hence both the N334-rCaT1 and the N198-rCaT1 function as inhibitors of CRAC activity in RBL mast cells.
Further, expression of the N302-TRPC3 fragment affected neither the activation nor the amount of endogenous CRAC currents in RBL mast cells (Fig. 6D–F) suggesting that the ankyrin-like repeats play a minor role in the inhibition of CRAC activity by the longer N-rCaT1 fragments.
In contrast to the two longer N-terminal fragments of rCaT1, expression of N154-rCaT1 in RBL mast cells clearly failed to affect the amount of CRAC activated (Fig. 7A–F). A small delay in the activation was observed in N154-rCaT1 expressing cells (Fig. 7A), but CRAC characteristics such as the current increase and its permeability properties as judged from the current–voltage relationships remained unchanged. Similar results were obtained when rCaT1 was coexpressed with N154-rCaT1 in RBL mast cells where store-operated rCaT1-derived currents were inhibited while endogenous CRAC currents remained unaffected (Fig. 7D–F). Hence, this N154-rCaT1 construct unequivocally discriminates between rCaT1 and CRAC currents.
To study the effects of the N-terminal fragments of rCaT1 in a more physiological context, Ca2+ fluorescence measurements (Fura-2) were performed on RBL mast cells stimulated by the Ca2+-ATPase inhibitor 2,5-di-t-butyl-1,4-hydrochinone (BHQ) (Fig. 8A, B and E–H) or immunologically by IgE plus antigen (Fig. 8C and D). RBL cells were initially stimulated in nominally Ca2+ free solution followed by the addition of Ca2+-containing extracellular solution which allows separation of release of intracellular Ca2+ from the entry of extracellular Ca2+. Release of Ca2+ from intracellular stores induced by BHQ was not altered by expression of N198-rCaT1 in RBL mast cells suggesting a target downstream of store depletion. Indeed, store-operated Ca2+ entry over the plasma membrane initiated by re-addition of extracellular Ca2+ was markedly reduced in these cells (Fig. 8A and B) consistent with the observed inhibition of CRAC currents as detected in electrophysiological experiments. Further, Ca2+ entry induced by immunological stimulation of RBL mast cells was inhibited by N198-rCaT1 (Fig. 8C and D). Moreover, the intracellular Ca2+ concentration in cells expressing N198-rCaT1 was slightly lower in nominally Ca2+ free solution as compared to control cells (Fig. 8A and C) suggesting inhibition of basal Ca2+ entry. However, Ca2+ entry in N154-rCaT1 expressing RBL cells, occurred to a similar extent as in mock-transfected cells (Fig. 8E and F) in accordance with the electrophysiological experiments.
Expression of the N302-TRPC3 affected neither Ca2+ release nor Ca2+ entry (Fig. 8G and H).
Yue et al. (2001) have suggested that CaT1 manifests the pore properties of CRAC channels and is activated by store depletion in CHO cells. In accordance with the concept of a link between CaT1 channels and intracellular Ca2+ stores, we have recently demonstrated store-dependent activation of CaT1 when expressed in RBL mast cells (Schindl et al. 2002). However, monovalent currents through CaT1 channels display a current–voltage relationship distinct from endogenous CRAC currents (Voets et al. 2001; Schindl et al. 2002), indicating that CRAC and CaT1 pore structures are not identical, which is further supported by a different ionic selectivity and single channel conductance (Voets et al. 2001; Prakriya & Lewis, 2002). Recently, a contribution of CaT1 to CRAC currents has been again suggested (Cui et al. 2002) as inferred from the suppression of endogenous CRAC activity in Jurkat T-lymphocytes when a pore mutant of CaT1 impermeable to Ca2+ is expressed. These authors have concluded that CaT1 is at least in part responsible for the native CRAC currents. The results of our present study shed light on this apparent discrepancy. The lack of effect of rCaT1 antisense and siRNA on endogenous CRAC currents in RBL mast cells together with an rCaT1 mRNA level below the detection limit as observed in this study renders it unlikely that rCaT1 is a subunit of native CRAC channels. However, we cannot completely exclude that knock-down strategies might be less efficient if the turnover of endogenous CaT1 as a component of CRAC channel complex is much slower than that of overexpressed CaT1 preventing the efficacy of our knock-down/dominant negative approaches.
The inhibition of CRAC currents in Jurkat T-lymphocytes by an expressed pore mutant of CaT1 (Cui et al. 2002) might be related to its interaction with CRAC channel proteins or within the activation pathway of both CRAC and CaT1 channels. We observed (unpublished results) a lack of effect of rCaT1 siRNA on Ca2+ entry in Jurkat cells in accordance with the results in RBL mast cells, and a similar inhibition with the N198-fragment of rCaT1, possibly assigning inhibition of CRAC currents by the expressed pore mutant of CaT1 (Cui et al. 2002) to structures in its N-terminus. Three N-terminal rCaT1 fragments (N334, N198 and N154) functioned as dominant negatives for rCaT1. While the N334- and N198-terminal fragments of rCaT1 were also identified as inhibitors of CRAC activity, the smallest N154-terminal fragment was ineffective indicating divergent structural requirements for CRAC and rCaT1 inhibition. Alternatively, the structural constraints of N-terminal fragments to act as dominant negative species might depend on the assembly of CaT1 in a homotetrameric or heterotetrameric form. The latter assembly could require the longer N-terminal fragments of CaT1 for inhibition, while the shortest N154-terminal strand might not posses an affinity high enough to disrupt a heteromultimeric CRAC/CaT1 channel complex. Nevertheless, store-operated Ca2+ current in LNCaP cells to which CaT1 proteins contribute (Vanden Abeele et al. 2003) was inhibited by all of our N-terminal rCaT1 fragments (authors' unpublished data).
The inhibition of CRAC activity by the two longer N-termini of rCaT1 is apparently not an unspecific, toxic effect, as endogenous inward rectifier and MagNuM currents of RBL mast cells were not significantly affected by the N198-rCaT1.
Our experiments provide important new insights in the CRAC phenomenon: (i) a contribution of CaT1 to CRAC current is very unlikely, and (ii) a novel mechanism of CRAC channel inhibition by an N-terminal structure of rCaT1. Hence this structure may provide an important tool for identification of molecular candidates of CRAC channels or of components regulating CRAC activity.
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We thank S. Buchegger and B. Kenda for excellent technical assistance and I. Graz for establishment of the Fura-2 measurements. This work was supported by projects FWF-F715 (SFB Biomembranes) and FWF-14950 (to K.G.), and FWF-15387, FWF-16537 and ÖNB 9343 (to C.R.)
Author's present address
J.-B. Peng: Division of Nephrology, University of Alabama Birmingham, Birmingham, AL 35294-0000, USA.