AJP - Heart Calcium Transients and Cell-Sarcomere
HOME HELP FEEDBACK SUBSCRIPTIONS ARCHIVE SEARCH TABLE OF CONTENTS
QUICK SEARCH:   [advanced]


     

Am J Physiol Heart Circ Physiol 282: H1229-H1236, 2002. First published November 29, 2001; doi:10.1152/ajpheart.00736.2001
0363-6135/02 $5.00
This Article
Right arrow Abstract Freely available
Right arrow Full Text (PDF)
Right arrow All Versions of this Article:
282/4/H1229    most recent
00736.2001v1
Right arrow Alert me when this article is cited
Right arrow Alert me if a correction is posted
Right arrow Citation Map
Services
Right arrow Email this article to a friend
Right arrow Similar articles in this journal
Right arrow Similar articles in Web of Science
Right arrow Similar articles in PubMed
Right arrow Alert me to new issues of the journal
Right arrow Download to citation manager
Citing Articles
Right arrow Citing Articles via HighWire
Right arrow Citing Articles via Web of Science (18)
Right arrow Citing Articles via Google Scholar
Google Scholar
Right arrow Articles by Li, P.-L.
Right arrow Articles by Campbell, W. B.
Right arrow Search for Related Content
PubMed
Right arrow PubMed Citation
Right arrow Articles by Li, P.-L.
Right arrow Articles by Campbell, W. B.
Vol. 282, Issue 4, H1229-H1236, April 2002

Role of ADP-ribose in 11,12-EET-induced activation of KCa channels in coronary arterial smooth muscle cells

Pin-Lan Li, David X. Zhang, Zhi-Dong Ge, and William B. Campbell

Departments of Pharmacology and Toxicology, Medical College of Wisconsin, Milwaukee, Wisconsin 53226


    ABSTRACT
TOP
ABSTRACT
INTRODUCTION
MATERIALS AND METHODS
RESULTS
DISCUSSION
REFERENCES

We recently reported that cADP-ribose (cADPR) and ADP-ribose (ADPR) play an important role in the regulation of the Ca2+-activated K+ (KCa) channel activity in coronary arterial smooth muscle cells (CASMCs). The present study determined whether these novel signaling nucleotides participate in 11,12-epoxyeicosatrienoic acid (11,12-EET)-induced activation of the KCa channels in CASMCs. HPLC analysis has shown that 11,12-EET increased the production of ADPR but not the formation of cADPR. The increase in ADPR production was due to activation of NAD glycohydrolase as measured by a conversion rate of NAD into ADPR. The maximal conversion rate of NAD into ADPR in coronary homogenate was increased from 2.5 ± 0.2 to 3.4 ± 0.3 nmol · min-1 · mg protein-1 by 11,12-EET. The regioisomers of 8,9-EET, 11,12-EET, and 14,15-EET also significantly increased ADPR production from NAD. Western blot analysis and immunoprecipitation demonstrated the presence of NAD glycohydrolase, which mediated 11,12-EET-activated production of ADPR. In cell-attached patches, 11,12-EET (100 nM) increases KCa channel activity by 5.6-fold. The NAD glycohydrolase inhibitor cibacron blue 3GA (3GA, 100 µM) significantly attenuated 11,12-EET-induced increase in the KCa channel activity in CASMCs. However, 3GA had no effect on the KCa channels activity in inside-out patches. 11,12-EET produced a concentration-dependent relaxation of precontracted coronary arteries. This 11,12-EET-induced vasodilation was substantially attenuated by 3GA (30 µM) with maximal inhibition of 57%. These results indicate that 11,12-EET stimulates the production of ADPR and that intracellular ADPR is an important signaling molecule mediating 11,12-EET-induced activation of the KCa channels in CASMCs and consequently results in vasodilation of coronary artery.

nicotinamide adenine dinucleotide glycohydrolase; K+ channels; epoxyeicosatrienoic acid; endothelium-derived hyperpolarization factor


    INTRODUCTION
TOP
ABSTRACT
INTRODUCTION
MATERIALS AND METHODS
RESULTS
DISCUSSION
REFERENCES

EPOXYEICOSATRIENOIC ACIDS (EETs), endothelium-derived arachidonic acid metabolites of cytochrome P-450, play an important role in the regulation of vascular tone (2, 13, 33, 48). In response to vasoactive substances such as acetylcholine, bradykinin, and arachidonic acid (AA), EETs are produced and released from endothelial cells of coronary, cerebral, and renal arteries (2, 31, 33, 48). EETs activate the Ca2+-activated K+ (KCa) channels, hyperpolarize vascular smooth muscle, and dilate vessels (9, 22, 23, 26, 31-33, 48), and therefore they are considered as endothelium-derived hyperpolarizing factors (2, 13). Recent studies in our laboratories and by others have shown that EETs induced activation of KCa channels by several membrane-limited mechanisms such as the activation of Gs protein via ADP-ribosylation (3, 9, 23, 35). However, the activity of KCa channels is also regulated by several different intracellular second messengers including cGMP and cAMP (8, 34). Although we demonstrated that adenylyl cyclase-cAMP and guanylyl cyclase-cGMP pathways are not involved in EETs-induced activation of KCa channels (2, 23), our studies did not exclude the role of other cytoplasmic factors in mediating the action of EETs.

Recently, endogenous metabolites of NAD, cADP-ribose (cADPR) and ADP-ribose (ADPR), have been identified as intracellular signaling molecules (10, 12, 19, 20, 25, 42). cADPR is formed from NAD via ADP-ribosylcyclase, and ADPR is produced by either hydrolysis of NAD via NAD glycohydrolase or hydrolysis of cADPR via cADPR hydrolase (14-16, 18, 25, 29). cADPR-mediated Ca2+ signaling participates in the regulation of a variety of cell functions or cellular activities (11, 12, 18, 21, 24, 28, 38, 40, 43). However, the physiological role of ADPR as a signaling molecule remains unknown. Because ADP-ribosylation, a transfer process of ADPR to protein, has been demonstrated to mediate the effect of EETs on the KCa channel activity (3, 23), it is possible that intracellular ADPR is also involved in the activation of KCa channel by EETs. Indeed, ADPR may cause nonenzymatic ADP-ribosylation of proteins, which regulates a number of biological events, including DNA repair, translational regulation of cellular protein, platelet aggregation, and gating of the fertilization channel in ascidian oocytes (6, 15, 36, 41). More recently, we (27) have reported that ADPR activates KCa channels in coronary arterial smooth muscle cells. Thus ADPR-induced KCa channel activation may contribute to the action of the EETs. The present study was designed to determine whether ADPR participates in 11,12-EETs-induced activation of the KCa channels in CASMCs. First, we determined the biochemical pathways for ADPR production and the effect of 11,12-EET on these pathways. Then we directly determined the role of ADPR in 11,12-EET-induced activation of the KCa channel using a patch-clamp technique and relaxation of coronary arteries by vascular reactivity studies.


    MATERIALS AND METHODS
TOP
ABSTRACT
INTRODUCTION
MATERIALS AND METHODS
RESULTS
DISCUSSION
REFERENCES

Preparation of homogenate from small bovine coronary arteries. Coronary arterial homogenates were prepared as we described previously (23). Briefly, bovine hearts were obtained from a local slaughterhouse. Small coronary arteries (250-300 µm) were microdissected under a dissecting stereomicroscope. These arteries were pooled and stored in ice-cold phosphate-buffered saline. The dissected coronary arteries were cut into very small pieces and homogenized with a glass homogenator in ice-cold HEPES buffer containing (in mmol/l) 25 Na-HEPES, 1 EDTA, 255 sucrose, and 0.1 phenylmethylsulfonyl fluoride. After centrifugation of the homogenized tissue at 6,000 g for 5 min at 4°C, the supernatant containing membrane and cytosolic components, termed homogenate, was aliquoted and frozen in liquid N2 and stored at -80°C until use.

Assay of NAD glycohydrolase in bovine coronary arterial homogenates. To determine the activity of NAD glycohydrolase, the homogenates (50 µg) were incubated for 60 min with 1 mmol/l NAD. All experiments were performed at 37°C in an assay buffer containing (in mmol/l) 250 potassium gluconate, 250 N-methylglucamine, 20 HEPES, and 1 MgCl2 (pH 7.2). The conversion rate of NAD into ADPR represents the NAD glycohydrolase activity. To determine the activity of cADPR hydrolase, the conversion rate of cADPR into ADPR was measured after incubation of the sample with cADPR (0.5 mM) at 37°C for 30 min. The total reaction volume was 0.1 ml. The reaction mixture was then rapidly frozen in liquid N2 to terminate the reaction. Before HPLC analysis, the reaction mixtures were centrifuged at 4°C using an Amicon microultrafilter at 13,000 rpm for 10 min to remove the proteins. HPLC analysis was performed as described previously (27, 43). To determine the effects of 8,9-EET, 11,12-EET, and 14,15-EET on the activity of NAD glycohydrolase, the coronary homogenates were preincubated with the EETs, and then NAD was added and incubated for 60 min. AA and 20-hydroxyeicosatetraenoic acid, an AA P-450 omega -hydrolase metabolite, (0.1 µmol/l), were used as a negative control.

Western blot analysis. Western blot was performed as described previously (23). Briefly, 30 µg of protein from the homogenates (microsomes or cytosols) were subjected to SDS-PAGE (12% running gel) after being heated at 100°C for 3 min. The protein was electrophoretically transferred onto a nitrocellulose membrane and then incubated with monoclonal antibody against human CD38 for 1 h at room temperature. CD38 possesses multiple enzyme activities including NAD glycohydrolase activity in a variety of tissues or cells (1, 4, 7, 14, 39, 45-47). After removal of the anti-CD38 antibody, the membrane was incubated for another 1 h with 1:1,000 horseradish peroxidase-labeled anti-mouse antibody. The detection solution 1 and 2 (1:1) (Amersham, IL) were added directly to the blots on the surface carrying the protein. After incubation for 1 min at room temperature, the membrane was wrapped in Saran Wrap and then exposed to Kodak Omat film.

Immunoprecipitation. Immunoprecipitation was performed as described previously (23). Briefly, the coronary arterial homogenate (140 µg) was incubated with the monoclonal antibody against CD38 (Pharmingen; San Diego, CA) for 18 h at 4°C. Samples were then incubated with protein A immobilized on Sepharose CL-4B beads (Sigma) for another 2 h at 4°C under constant rotation. Beads and supernatant were separated by centrifugation at 12,000 g for 5 min. Western blotting was used to confirm the removal of CD38. The supernatant was used to measure the activity of NAD glycohydrolase by HPLC.

Patch-clamp study. Smooth muscle cells were prepared, and the patch-clamp study was performed as we described previously (22). The bath solutions used for single channel recordings in the cell-attached mode contained (in mmol/l) 145 KCl, 1.8 CaCl2, 1.1 MgCl2, 10 glucose, and 5 HEPES (pH 7.4), and the pipette solution contained (in mmol/l) 145 KCl, 1.8 CaCl2, 1.1 MgCl2, and 5 HEPES (pH 7.4). The bath solutions used for single channel recordings in the inside-out excised membrane patch contained (in mmol/l) 145 KCl, 1.1 MgCl2, 10 HEPES, 2 EGTA, and 300 nmol/l ionized calcium (pH 7.2), and the pipette solution contained (in mmol/l) 145 KCl, 1.8 CaCl2, 1.1 MgCl2, and 10 HEPES, 10 (pH 7.4).

The effects of the specific NAD glycohydrolase inhibitor, cibacron 3GA (3GA, 1-100 µmol/l) (17), on the KCa channel activity was determined in the presence or absence of 11,12-EET. After a cell-attached patch was established, a 3-min control recording was obtained at a membrane potential of +40 mV. The bath solution was then changed to contain 3GA (1-100 µmol/l), and a second successive 3-min recording at each concentration was obtained. To determine the effects of these inhibitors on 11,12-EETs-induced activation of the K+ channels, patch-clamp recordings were performed in the cell-attached patch mode. A 3-min control recording was obtained at a membrane potential of +40 mV. The bath solution was then exchanged with the solution containing 11,12-EET (100 nmol/l) (n = 6), and then a second successive 3-min recording was obtained. In another group of cells, 3GA (100 µmol/l) was added into the bath solution. A 3-min control recording was obtained at a membrane potential of +40 mV. The solution in the bath was then exchanged with the solution containing 11,12-EET (100 nmol/l), and then a second successive 3-min recording was obtained (n = 6).

The inside-out patch mode was used to further determine the effects of 3GA on the activity of the K+ channels. After inside-out patches were established, a 3-min control recording was obtained at a membrane potential of +40 mV (n = 5). 3GA (100 µmol/l) was then added into the bath solution, and another 3-min control recording was obtained at the same membrane potential as above (n = 5).

Vascular reactivity studies. Vascular reactivity in bovine coronary arteries was determined as we described previously (11, 44). Briefly, the epicardial left anterior descending coronary artery was dissected and placed in a Krebs bicarbonate solution. The rings were prepared and suspended in a 6-ml water-jacked organ chamber at 37°C. The contractile responses were monitored using a computerized recording system. After an equilibration period of 1.5 h, the vessels were activated by addition of KCl (80 mmol/l) until reproducible contractions were obtained. One ring of each pair then received a vehicle (0.01% ethanol), and other ring received 3GA (30 µmol/l, n = 12) for 15 min before the addition of the thromboxane mimetic U-46619 (20 nmol/l). After a sustained contraction by U-46619 was obtained, cumulative additions of 11,12 EET (10-9 to 10-5 M) were made every 4 min until a plateau response was reached. 11,12-EET-induced vasodilation was evaluated in the presence or absence of 3GA.

To further determine the effect of inhibition of ADPR production on 11,12-EET-induced relaxation of resistance coronary arteries, these small coronary arteries (250-300 µm) were preconstricted by 50 ± 10% of their resting diameter with the thromboxane A2 analog U-46619. Once steady-state contraction was obtained, cumulative dose-response curves of 11,12-EET (0.1 nmol/l to 1 µmol/l) or sodium nitroprusside (SNP, 10 nmol/l to 100 µmol/l) were determined by measuring changes in the internal diameter. In another group of experiments, the arteries were preincubated with NAD glycohydrolase inhibitor 3GA (30 µmol/l), and the concentration-dependent response of the arteries to 11,12-EET or SNP were measured. During the whole experiments, physiological saline solution in the bath was continuously bubbled with a gas mixture of 95% O2-5% CO2 and maintained at 37 ± 0.1°C (44).

Statistical analysis. Data were presented as means ± SE. Significance of differences in mean values within and between multiple groups was examined using two-way ANOVA for repeated measures followed by a Duncan's multiple range test. A Student's t-test was used to examine significance of difference in two groups. P < 0.05 is considered statistically significant.


    RESULTS
TOP
ABSTRACT
INTRODUCTION
MATERIALS AND METHODS
RESULTS
DISCUSSION
REFERENCES

Effect of 11,12-EET on the activity of NAD glycohydrolase. Figure 1 presents a representative reverse-phase HPLC chromatogram depicting the metabolism of NAD by coronary arterial homogenates. When the homogenates were incubated with NAD, products with retention times of 3.1 and 15.6 min coeluted with synthetic cADPR and ADPR, respectively (Fig. 1A). In the presence of 11,12-EET (100 nmol/l), ADPR production was markedly increased (Fig. 1B). The conversion rate of NAD into ADPR was increased from 2.54 ± 0.2 nmol · min-1 · mg protein-1 of control to 3.43 ± 0.3 nmol · min-1 · mg protein-1 in the presence of 100 nmol/l 11,12-EET. However, 11,12-EET had no effect on the production of cADPR (Fig. 1C).


View larger version (19K):
[in this window]
[in a new window]
  		Fig. 1.   HPLC analysis of cADP-ribose (cADPR) and ADP-ribose (ADPR) produced by homogenates of bovine coronary arteries in the presence of NAD (1 mmol/l). A: typical HPLC chromatogram showing production of cADPR and ADPR (control). B: production of cADPR and ADPR in coronary artery homogenates in the presence of 11,12-epoxyeicosatrienoic acid (11,12-EET, 100 nmol/l). C: summarized data showing the effect of 11,12-EET on the conversion rate of NAD into cADPR and ADPR, which represents activity of ADP-ribosylcyclase and NAD glycohydrolase in coronary arteries. *Significant difference from control (P < 0.05, n = 20).

To detect the effects of EET regioisomers, AA, and other AA metabolites on the NAD glycohydrolase, the coronary arterial homogenates were incubated with NAD in the presence of 8,9-EET, 11,12-EET, 14,15-EET, AA, or 20-HETE. As shown in Fig. 2, all three of the EETs significantly increased the conversion rate of ADPR. However, AA and 20-HETE had no effect on the synthesis of ADPR.


View larger version (16K):
[in this window]
[in a new window]
  		Fig. 2.   Effects of EETs, archidonic acid (AA), and 20,15-hydroxyeicosatetraenoic acid (20-HETE) (0.1 µmol/l) on the conversion rate of NAD into ADPR, which represents activity of NAD glycohydrolase, in coronary arteries. *Significant difference from control (P < 0.05, n = 9).

Effect of immunoprecipitation of CD38 on 11,12-EET-induced increase in the NAD glycohydrolase activity. Figure 3A presents a typical Western blot analysis of CD38 in coronary arteries. As indicated above, CD38 possesses NAD glycohydrolase activity. Two immunoreactive bands with molecular sizes of 42 and 90 kDa were recognized by a monoclonal antibody against CD38 in coronary arterial homogenates (Fig. 3A, lane H), microsomes (lane M), and cytosol (lane C). A purified calf spleen NAD glycohydrolase (lane N) and cell lysate from human white blood cells (lane W) were analyzed at same time as a positive control, and only one band with 42 kDa was recognized by this antibody. The identity of a 90-kDa immunoreactive band in bovine coronary arterial preparations was not clarified. Previous studies have reported that this band may be an oxidized dimer of CD38 (1). It is possible that we have detected this dimerized CD38 in coronary arteries, but not in purified CD38 or human white blood cells. The effect of removing CD38 from the homogenates of coronary arterial smooth muscle on NAD glycohydrolases activity was examined on the production of ADPR by HPLC analysis. 11,12-EET significantly increased the production of ADPR in coronary arterial muscle homogenates under control condition. After the removal of CD38 by immunoprecipitation, the basal activity of NAD glycohydrolase (-CD38) was significantly decreased, and 11,12-EET-induced increase in NAD glycohydrolase activity (-CD38 + EET) was completely blocked (Fig. 3B).


View larger version (42K):
[in this window]
[in a new window]
  		Fig. 3.   A: Western blot analysis of CD38 in homogenates (lane H), microsomes (lane M), and cytosols (lane C) prepared from small bovine coronary arteries and purified calf spleen NAD glycohydrolase (lane N) and human white blood cells (lane W). B: effect of removal CD38 (-CD38, n = 19) on the conversion rate of ADPR in homogenates of bovine coronary arteries. *Significant difference from the value obtained before removal of CD38 (P < 0.05).

Effect of 3GA on the activity of NAD glycohydrolase. Figure 4A shows the effect of 3GA on the activity of NAD glycohydrolase and cADPR hydrolase. 3GA significantly decreased the production of ADPR in a concentration-dependent manner. The conversion rate of NAD to ADPR, which represented NAD glycohydrolase activity, was 3.028 ± 0.03 nmol · min-1 · mg protein-1 in control versus 0.48 ± 0.17 nmol · min-1 · mg protein-1 in the presence of 100 µmol/l 3GA, a 84% reduction. However, 3GA had no effect on the activity of cADPR hydrolase (Fig. 4A). As shown in Fig. 4B, the production of ADPR was markedly increased in the presence of 11,12-EET (100 nmol/l). However, 3GA at 100 µmol/l significantly attenuated the 11,12-EET-induced increase in the production of ADPR. The conversion rate of NAD into ADPR was decreased from 4.42 ± 0.33 nmol · min-1 · mg protein-1 in the presence of 100 nmol/l 11,12-EET to 2.6 ± 0.47 nmol · min-1 · mg protein-1 after the addition of 3GA and 11,12-EET (Fig. 4B).


View larger version (24K):
[in this window]
[in a new window]
  		Fig. 4.   A: effect of cibacron blue 3GA (3GA) on the activity of NAD glycohydrolase and cADPR hydrolase. B: effect of 3GA on 11,12-EET-induced activation of NAD glycohydrolase. *Significant difference from control. #Significant difference from the 11,12-EET treatment only (P < 0.05, n = 6-9).

Effect of inhibition of NAD glycohydrolase on 11,12-EET-induced increase of KCa channel activity. Figure 5A presents typical recording of KCa channels in cell-attached patches, depicting the effect of NAD glycohydrolase inhibitor 3GA (100 µmol/l) on the 11,12-EET-induced activation of KCa channel. As in previous studies, 11,12-EET (100 nmol/l) increases the KCa channel activity by 5.6-fold (Fig. 5, A and C). 3GA alone decreases the activity of KCa channel in a concentration-dependent manner (Fig. 5B). In the presence of 3GA, the 11,12-EET-induced increases in opening of KCa channel were completely blocked. 3GA had no effect on KCa channels in inside-out patches (open probability = 0.043 ± 0.01 of control vs. 0.043 ± 0.01 with 100 µmol/l 3GA).


View larger version (29K):
[in this window]
[in a new window]
  		Fig. 5.   A: representative recordings depicting the effects of 11,12-EET (100 nmol/l) and 3GA on the Ca2+-activated K+ (KCa) channel activity in the cell-attached patches. B: effect of 3GA alone on the open probablility (NPO) of the KCa channels. C: effects of 3GA (100 µmol/l) on 11,12-EET-induced activation of the KCa channels. *Significant difference from control; #Significant difference from the 11,12-EET treatment only (P < 0.05, n = 20).

Effect of inhibition of NAD-glycohydrolase on 11,12-EET-induced relaxation of bovine coronary artery. Figure 6A shows that 11,12-EET produced a concentration-dependent relaxation in U-46619-precontracted coronary arterial rings. The maximal relaxation (92%) to 11,12-EET occurred at 10 µmol/l. Pretreatment of coronary arterial rings with NAD glycohydrolase inhibitor, 3GA (30 µmol/l) markedly attenuated 11,12-EET-induced relaxation by 41%. In microperfused and pressurized small coronary arteries, 11,12-EET was found to relax these resistance arteries even at 1 nmol/l (Fig. 6B). In the presence of 3GA, 11,12-EET-induced vasodilation was significantly decreased. However, 3GA had no effect on SNP-induced vasodilation (Fig. 6C).


View larger version (16K):
[in this window]
[in a new window]
  		Fig. 6.   A: effect of 3GA (30 µmol/l) on 11,12-EET-induced vasorelaxation of bovine epicardial left anterior descending coronary artery with diameter of 2-3 mm (n = 12). B: effect of 3GA (30 µmol/l) on 11,12-EET-induced vasorelaxation of small bovine coronary artery with diameter of 250-300 µm (n = 7). C: effect of 3GA (30 µmol/l) on sodium nitroprusside (SNP)-induced vasorelaxation of small bovine coronary artery with diameter of 250-300 µm (n = 5). *Significant difference from the values obtained during addition of 11,12-EET alone (P < 0.05).


    DISCUSSION
TOP
ABSTRACT
INTRODUCTION
MATERIALS AND METHODS
RESULTS
DISCUSSION
REFERENCES

NAD glycohydrolase converts NAD to ADPR (15-17, 29, 41, 44). Because ADPR increases KCa channel activity (27), we were interested in the regulation of the synthesis of ADPR and its signaling action in the coronary arterial smooth muscle. Using HPLC analysis, we found that homogenates from coronary arterial smooth muscle metabolized NAD to ADPR. The conversion rate of NAD to ADPR was significantly increased by 11,12-EET. Moreover, 8,9-EET, 11,12-EET, and 14,15-EET had similar stimulatory effects on the NAD glycohydrolase activity in the vascular smooth muscle. However, AA and 20-HETE, another cytochrome P-450 metabolite of AA, did not activate this enzyme. These results provide the first evidence indicating that NAD glycohydrolase may be an enzymatic target of EETs in coronary arterial smooth muscle and that EETs activate the NAD glycohydrolase to increase intracellular ADPR concentrations.

CD38 possesses NAD glycohydrolase activity in a variety of mammalian tissues or cells (1, 4, 7, 14, 39, 45-47). In the present study, CD38 was detected in coronary arteries by Western blot analysis. After removal of CD38 from coronary homogenates by immunoprecipitation, 11,12-EET-induced production of ADPR was significantly blocked. These results indicate that in bovine coronary arterial smooth muscle, 11,12-EET increases ADPR production through CD38-associated NAD glycohydrolase activity.

A selective inhibitor of NAD glycohydrolase 3GA attenuated basal activity of NAD glycohydrolase and also blocked 11,12-EET-induced increase of NAD glycohydrolase activity. These results further support the view that 11,12-EET-induced production of ADPR is due to the activation of NAD glycohydrolase. We performed patch-clamp experiments to examine the effect of 3GA on the activity of KCa channels in cell-attached patches. 3GA decreased the basal activity of KCa channels and completely abolished 11,12-EET-induced activation of the KCa channel. However, in the inside-out patches, 3GA has no effect on the KCa channel. These results suggested that 11,12-EET-induced activation of KCa channels is through the activation of NAD glycohydrolase, which depends on the presence of cellular soluble substrate NAD. To further define the role of ADPR in 11,12-EET-induced vasorelaxation, vascular reactivity to 11,12-EET was examined in the absence or presence of 3GA. In the presence of 3GA, 11,12-EET-induced vasorelaxation was attenuated in both epicardial coronary arteries and small coronary arteries. However, 3GA had no effect on SNP-induced vasorelaxation. This suggests that ADPR may mediate 11,12-EET-induced activation of KCa channels in bovine coronary arterial smooth muscle and consequently result in vasorelaxation of these vessels. There is increasing evidence that NAD metabolites mediate the effects of a number of agonists in tissues or cells (45-47). In pancreatic beta -cells, an ADP-ribosylcyclase product of NAD, cADPR mediates glucose-induced insulin secretion (38). cADPR may also mediate the effects of the activation of acetylcholine receptors in adrenal chromaffin cells, estrogen receptors in uterus, 5-hydroxytryptamine 2B receptors in arterial endothelial cells, and retinoic acid in renal tubular cells and aortic smooth muscle (5, 28, 37, 40). The present findings indicate that another NAD metabolite, ADPR may also serve as a signaling molecule, which mediates the effects of 11,12-EETs on coronary arterial smooth muscle. This role of ADPR in mediating the effect of EETs may represent a new signaling pathway regulating the activity of KCa channels and the action of endothelium-derived hyperpolarizing factors.

We have previously reported a role for Gsalpha in mediating 11,12-EET-induced activation of the KCa channels (22). 11,12-EET stimulated the endogenous ADP-ribosylation of GS, and the activation of GS increased the activity of KCa channels. In other studies, EETs activated KCa channel through a Gs-mediated, membrane-delimited effect in HEK293 cells (9), which is consistent with our findings. The present study demonstrated that 11,12-EET activated NAD glycohydrolase, increased intracellular ADPR, and thereby induced activation of the KCa channels, resulting in the relaxation of coronary arteries. These results indicate that a cytoplasmic signaling nucleotide ADPR may mediate the EET effect. Therefore, the mechanisms mediating the action of EETs on KCa channel activity may be associated not only with ADP-ribosylation of GS, but also with ADPR-mediated activation of these channels.

In summary, the present study demonstrates that NAD glycohydrolase present in bovine coronary arterial smooth muscle catalyzes the hydrolysis of NAD into ADPR. 11,12-EET activates KCa channels by increasing the production of ADPR through the activation of NAD glycohydrolase in coronary arterial smooth muscle. These results suggest that NAD glycohydrolase product, ADPR participates in the regulation of the activity of KCa channels in coronary vascular smooth muscle. ADPR may serve as intracellular second messenger mediating 11,12-EET-induced activation of the KCa channels. Therefore, ADPR may play a role in mediating endothelium-dependent hyperpolarization in the coronary circulation.


    ACKNOWLEDGEMENTS

The authors thank Gretchen Barg for secretarial assistance and Sarah Hittner for technical help.


    FOOTNOTES

First published November 29, 2001;10.1152/ajpheart.00736.2001

This study was supported by National Heart, Lung, and Blood Institute Grants HL-57244 and HL-51055, and P.-L. Li is a recipient of Established Investigator Award 9940167N from the American Heart Association.

Address for reprint requests and other correspondence: P.-L. Li, Dept. of Pharmacology and Toxicology, Medical College of Wisconsin, 8701 Watertown Plank Rd., Milwaukee, WI 53226 (E-mail: pli{at}post.its.mcw.edu).

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.

Received 17 August 2001; accepted in final form 21 November 2001.


    REFERENCES
TOP
ABSTRACT
INTRODUCTION
MATERIALS AND METHODS
RESULTS
DISCUSSION
REFERENCES

1.   Berruet, L, Muller-Steffner H, and Schuber F. Occurrence of bovine spleen CD38/NAD+ glycohydrolase disulfide-linked dimer. Biochem Mol Biol Int 46: 847-855, 1998.

2.   Campbell, WB, Gebremedhin D, Pratt PF, and Harder DR. Identification of epoxyeicosatrienoic acid as endothelium-derived hyperpolarizing factors. Circ Res 78: 415-423, 1996.

3.   Campbell, WB, Zou AP, and Li PL. Epoxyeicosatrienoic acid as endothelium-derived hyperpolarization factors in coronary arteries: potassium channels activation through endogenous ADP-ribosylation of Gs. In: Endothelium-Dependent Hyperpolarizations, edited by Vanhoutte PM.. Amsterdam, the Netherlands: Harwood Academic, 2000, p. 11-16.

4.   Chidambaram, N, Wong ET, and Chang CF. Differential oligomerization of membrane-bound CD38/ADP-ribosyl cyclase in porcine heart microsomes. Biochem Mol Biol Int 44: 1225-1233, 1998.

5.   Chini, EN, de Toledo FG, Thompson MA, and Dousa TP. Effect of estrogen upon cyclic ADP-ribose metabolism: beta -estradiol stimulates ADP ribosyl cyclase in rat uterus. Proc Natl Acad Sci USA 94: 5872-5876, 1997.

6.   Del Principe, D, Menichelli A, Casini A, Di Giulio S, Mancuso G, and Finazzi-Agro A. A surface NAD-glycohydrolase of human platelet may influence their aggregation. FEBS Lett 205: 66-70, 1986.

7.   Franco, L, Zocchi E, Calder L, Guida L, Benatti U, and De Flora A. Self-aggregation of the transmembrane glycoprotein CD38 purified from human erythrocytes. Biochem Biophys Res Commun 202: 1710-1715, 1994.

8.   Fukao, M, Mason HS, Britton FC, Kenyon JL, Horowitz B, and Keef KD. Cyclic GMP-dependent protein kinase activates cloned BKCA channels expressed in mammalian cells by direct phosphorylation at serine 1072. J Biol Chem 274: 10927-10935, 1999.

9.   Fukao, M, Mason HS, Kenyon JL, Horowitz B, and Keef KD. Regulation of BKCa channels expressed in human embryonic kidney 293 cells by epoxyeicosatrienoic acid. Mol Pharmacol 59: 16-23, 2001.

10.   Galione, A. Cyclic ADP-ribose, the ADP-ribosyl cyclase pathway and calcium signaling. Mol Cell Endocrinol 98: 125-131, 1994.

11.   Geiger, J, Zou AP, Campbell WB, and Li PL. Inhibition of cyclic ADP-ribose formation produces vasodilation in bovine coronary arteries. Hypertension 35: 397-402, 2000.

12.   Guse, AH. Cyclic ADP-ribose. J Mol Med 78: 26-35, 2000.

13.   Hecker, M, Bara AT, Bauersachs J, and Busse R. Characterization of endothelium-derived hyperpolarizing factor as a cytochrome P450-derived arachidonic acid metabolite in mammals. J Physiol (Lond) 481: 407-414, 1994.

14.   Howard, M, Grimaldi JC, Bazan JF, Lund FE, Santos-Argumedo L, Parkhouse RM, Walseth TF, and Lee HC. Formation and hydrolysis of cyclic ADP-ribose catalyzed by lymphocyte antigen CD38. Science 262: 1056-1059, 1993.

15.   Hilz, H. ADP ribose. A historical overview. Adv Exp Med Biol 419: 15-24, 1997.

16.   Kim, H, Jacobson EL, and Jacobson MK. Synthesis and degradation of cyclic ADP-ribose by NAD glycohydrolases. Science 261: 1330-1333, 1993.

17.   Kim, UH, Kim MK, Kim JS, Han MK, Park BH, and Kim HR. Purification and characterization of glycohydrolase from rabbit erythrocytes. Arch Biochem Biophys 305: 147-152, 1993.

18.   Lee, HC, and Aarhus R. ADP-ribosyl cyclase: an enzyme that cyclase NAD+ into a calcium-mobilizing metabolite. Cell Regul 2: 203-209, 1991.

19.   Lee, HC, Walseth TF, Aarhus R, and Levitt D. Cyclic ADP-ribose as a second messenger for mobilizing intracellular calcium stores. J Reprod Devel 39: 64-69, 1993.

20.   Lee, HC, Walseth TF, Bratt GT, Hayes RN, and Clapper DL. Structural determination of a cyclic metabolite of NAD+ with intracellular Ca2+-mobilizing activity. J Biol Chem 264: 1608-1615, 1989.

21.   Li, N, Teggatz EG, Li PL, Allaire R, and Zou AP. Formation and actions of cyclic ADP-ribose in renal microvessels. Microvasc Res 60: 149-159, 2000.

22.   Li, PL, and Campbell WB. Epoxyeicosatrienoic acids activate potassium channels in coronary smooth muscle through a guanine nucleotide binding protein. Circ Res 80: 877-884, 1997.

23.   Li, PL, Chen CL, Bortel R, and Campbell WB. 11,12-Epoxyeicosatrienoic acids stimulates endogenous mono-ADP-ribosylation in bovine coronary arterial smooth muscle. Circ Res 85: 349-356, 1999.

24.   Li, PL, Tang WX, Valdivia HH, Zou AP, and Campbell WB. cADP-ribose activates reconstituted ryanodine receptors from coronary arterial smooth muscle. Am J Physiol Heart Circ Physiol 280: H208-H215, 2001.

25.   Li, PL, Zou AP, and Campbell WB. Metabolism and actions of ADP-riboses in coronary arterial smooth muscle. Adv Exp Med Biol 419: 437-441, 1997.

26.   Li, PL, Zou AP, and Campbell WB. Regulation of potassium channels in coronary arterial smooth muscle by endothelium-derived vasodilators. Hypertension 29: 262-267, 1997.

27.   Li, PL, Zou AP, and Campbell WB. Regulation of the KCa channel activity by cADP-ribose and ADP-ribose in bovine coronary arterial smooth muscle. Am J Physiol Heart Circ Physiol 275: H1002-H1010, 1998.

28.   Morita, K, Kitayama S, and Dohi T. Stimulation of cyclic ADP-ribose synthesis by acetylcholine and its role in catecholamine release in bovine adrenal chromaffin cells. J Biol Chem 272: 21002-21009, 1997.

29.   Muller-Steffner, H, Muzard M, Oppenheimer N, and Schuber F. Mechanistic implications of cyclic ADP-ribose hydrolysis and methanolysis catalyzed by calf spleen NAD+ glycohydrolase. Biochem Biophys Res Commun 204: 1279-1285, 1994.

30.   Okamota, H. The CD38-cyclic ADP-ribose signal system: molecular mechanism and biological significance. Nippon Yakurigaku Zasshi 114: 131-139, 1999.

31.   Oltman, CL, Weintraub NL, VanRollins M, and Dellsperger KC. Epoxyeicosatrienoic acids and dihydroxyeicosatrienoic acids are potent vasodilators in the canine coronary microcirculation. Circ Res 83: 932-939, 1998.

32.   Pratt, PF, Li PL, Kurian J, and Campbell WB. Endotheium-independent, ouabain-sensitive relaxation of bovine coronary atrteries by epoxyeicosatrienoic acids. Am J Physiol Heart Circ Physiol 280: H1113-H1121, 2001.

33.   Rosolowsky, M, and Campbell WB. Role of PGI2 and EETs in the relaxation of bovine coronary arteries to arachidonic acid. Am J Physiol Heart Circ Physiol 264: H327-H335, 1993.

34.   Scornik, FS, Codina J, Birnbaumer L, and Toro L. Modulation of coronary smooth muscle KCa channels by GSalpha independent of phosphorylation by protein kinase A. Am J Physiol Heart Circ Physiol 265: H1460-H1465, 1993.

35.   Seki, K, Hirai A, Noda M, Tamura Y, Kato I, and Yoshida S. Epoxyeicosatrienoic acid stimulates ADP-ribosylation of a 52-kDa protein in rat liver cytosol. Biochem J 281: 185-190, 1992.

36.   Shall, S. ADP ribosylation reactions. Biochimie 77: 313-318, 1995.

37.   Takahashi, K, Kukimoto I, Tokita K, Inageda K, Inoue S, Kontani K, Hoshino S, Nishina H, Kanaho Y, and Katada T. Accumulation of cyclic ADP-ribose measured by a specific radioimmunoassay in differentiated human leukemic HL-60 cells with alltransretinoic acid. FEBS Lett 371: 204-208, 1995.

38.   Takesawa, S, Nata K, Yonekura H, and Okamoto H. Cyclic ADP-ribose in insulin secretion from pancreatic cells. Science 259: 370-373, 1993.

39.   Tohgo, A, Takasawa S, Noguchi N, Koguma T, Nata K, Sugimoto T, Furuya Y, Yonekura H, and Okamoto H. Essential cysteine residues for cyclic ADP-ribose synthesis and hydrolysis by CD38. J Biol Chem 269: 28555-28557, 1994.

40.   Ullmer, C, Boddeke HG, Schmuck K, and Lubbert H. 5-HT2B receptor-mediated calcium release from ryanodine-sensitive intracellular store in human pulmonary artery endothelial cells. Br J Pharmacol 117: 1081-1088, 1996.

41.   Wilding, M, Russo GL, Galione A, Marino M, and Dale B. ADP-ribose gates the fertilization channel in ascidian oocytes. Am J Physiol Cell Physiol 275: C1277-C1283, 1998.

42.   White, AM, Watson SP, and Galione A. Cyclic ADP-ribose-induced Ca2+ release from rat brain microsomes. FEBS Lett 318: 259-263, 1993.

43.   Yu, JZ, Zhang DX, Zou AP, Campbell WB, and Li PL. Nitric oxide inhibits Ca2+ mobilization through cADP-ribose signaling in coronary arterial smooth muscle cells. Am J Physiol Heart Circ Physiol 279: H873-H881, 2000.

44.   Zhang, DX, Zou AP, and Li PL. ADP-ribose dilates coronary arteries through apyrase-mediated metabolism. J Vasc Res 38: 64-72, 2001.

45.   Zocchi, E, Franco L, Guida L, Benatti U, Bragellesi A, Malavasi F, Lee HC, and De Flora A. A single protein immunologically identified as CD38 displays NAD+ glycohydrolase, ADP-ribosyl cyclase and cyclic ADP-ribose hydrolase activities at the outer surface of human erythrocytes. Biochem Biophys Res Commun 196: 1459-1465, 1993.

46.   Zocchi, E, Franco L, Guida L, Calder L, and De Flora A. Self-aggregation of purified and membrane-bound erythrocyte CD38 induces extensive decrease of its ADP-ribosyl cyclase activity. FEBS Lett 359: 35-40, 1995.

47.   Zocchi, E, Usai C, Guida L, Franco L, Bruzzone S, Passalacqua M, and de Flora A. Ligand-induced internalization of CD38 results in intracellular Ca2+ mobilization: role of NAD+ transport across cell membranes. FASEB J 13: 273-283, 1999.

48.   Zou, AP, Fleming JT, Falck JR, Jacobs ER, Gebremedhin D, Harder DR, and Roman RJ. Stereospecific effect of 11,12-epoxyeicosatrienoic acid on vascular tone and K+-channel activity of renal arterioles in rats. Am J Physiol Renal Fluid Electrolyte Physiol 270: F822-F832, 1996.

Am J Physiol Heart Circ Physiol 282(4):H1229-H1236
0363-6135/02 $5.00 Copyright © 2002 the American Physiological Society


This article has been cited by other articles:


Home page
 Exp PhysiolHome page
H. C. Hercule, B. Salanova, K. Essin, H. Honeck, J. R. Falck, M. Sausbier, P. Ruth, W.-H. Schunck, F. C. Luft, and M. Gollasch
Vascular: The vasodilator 17,18-epoxyeicosatetraenoic acid targets the pore-forming BK {alpha} channel subunit in rodents
Exp Physiol, November 1, 2007; 92(6): 1067 - 1076.
[Abstract] [Full Text] [PDF]

Home page
 Am. J. Physiol. Renal Physiol.Home page
M. A. Carroll, A. B. Doumad, J. Li, M. K. Cheng, J. R. Falck, and J. C. McGiff
Adenosine2A receptor vasodilation of rat preglomerular microvessels is mediated by EETs that activate the cAMP/PKA pathway
Am J Physiol Renal Physiol, July 1, 2006; 291(1): F155 - F161.
[Abstract] [Full Text] [PDF]

Home page
 Am. J. Physiol. Renal Physiol.Home page
J. D. Imig
Epoxide hydrolase and epoxygenase metabolites as therapeutic targets for renal diseases
Am J Physiol Renal Physiol, September 1, 2005; 289(3): F496 - F503.
[Abstract] [Full Text] [PDF]

Home page
 J. Lipid Res.Home page
V. Le Quere, E. Plee-Gautier, P. Potin, S. Madec, and J.-P. Salaun
Human CYP4F3s are the main catalysts in the oxidation of fatty acid epoxides
J. Lipid Res., August 1, 2004; 45(8): 1446 - 1458.
[Abstract] [Full Text] [PDF]

This Article
Right arrow Abstract Freely available
Right arrow Full Text (PDF)
Right arrow All Versions of this Article:
282/4/H1229    most recent
00736.2001v1
Right arrow Alert me when this article is cited
Right arrow Alert me if a correction is posted
Right arrow Citation Map
Services
Right arrow Email this article to a friend
Right arrow Similar articles in this journal
Right arrow Similar articles in Web of Science
Right arrow Similar articles in PubMed
Right arrow Alert me to new issues of the journal
Right arrow Download to citation manager
Citing Articles
Right arrow Citing Articles via HighWire
Right arrow Citing Articles via Web of Science (18)
Right arrow Citing Articles via Google Scholar
Google Scholar
Right arrow Articles by Li, P.-L.
Right arrow Articles by Campbell, W. B.
Right arrow Search for Related Content
PubMed
Right arrow PubMed Citation
Right arrow Articles by Li, P.-L.
Right arrow Articles by Campbell, W. B.

HOME HELP FEEDBACK SUBSCRIPTIONS ARCHIVE SEARCH TABLE OF CONTENTS
Visit Other APS Journals Online