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PACAP peptides are expressed in micturition pathways and PACAP expression is regulated by urinary bladder inflammation. Previous physiological studies have demonstrated roles for PACAP27 and PACAP38 in detrusor smooth muscle (DSM) contraction and a PAC1 receptor antagonist reduced cyclophosphamide (CYP)-induced bladder hyperreflexia. To gain insight into PACAP signaling in micturition and regulation with cystitis, receptor characterization by real time quantitative polymerase chain reaction and physiological assays were performed. PACAP receptors were identified in tissues of rat micturition pathway, including DSM, urothelium (U) and dorsal root ganglia (DRG) after acute (4 hr), intermediate (48 hr) or chronic (8 day) CYP-induced cystitis. PAC1 mRNA expression significantly (p ≤ 0.05) increased in U and DSM after 48 hr and chronic CYP-induced cystitis after an initial decrease at 4 hr. VPAC1 and VPAC2 transcripts increased in U and DSM after acute and intermediate CYP-induced cystitis followed by a decrease in VPAC2 expression with chronic cystitis. Application of PACAP27 (100 nM) to cultured urothelial cells evoked ATP release that was blocked by the PAC1 specific antagonist, M65 (1 µM). PACAP38 (100 nM) also evoked ATP release from cultured urothelial cells but ATP release was less than that observed with PACAP27. PACAP transcripts were increased in the U with intermediate and chronic cystitis whereas VIP expression in both tissues was very low and showed no regulation with cystitis. Regulation of PACAP, galanin and substance P transcripts expression was observed in lumbosacral DRG but no regulation for VIP was observed. The current data demonstrate PACAP and PAC1 regulation in micturition pathways with inflammation and PACAP-mediated ATP release from urothelium.
Pain and micturition dysfunction in interstitial cystitis (IC) or painful bladder syndrome (PBS) may involve an alteration in bladder sensory neuron and urinary bladder function. Many studies have suggested the involvement of the neuropeptide, pituitary adenylate cyclase activating polypeptide (PACAP) in lower urinary tract function after bladder inflammation (Vizzard, 2000c; Braas et al., 2006; Herrera et al., 2006) or spinal cord injury (Zvarova et al., 2005; Zvara et al., 2006;). PACAP is a member of the vasoactive intestinal polypeptide (VIP), secretin, glucagon family of hormones and exhibits ~68% homology to VIP (Arimura, 1992). PACAP can act on three types of G protein-coupled receptors including VPAC1 and VPAC2 that respond to PACAP and VIP whereas PAC1 is a specific receptor for PACAP (Arimura, 1998; Sherwood et al., 2000; Vaudry et al., 2000).
Dense PACAP-immunoreactive sensory fibers are found within the bladder wall and suburothelial plexus (Fahrenkrug and Hannibal, 1998; Mohammed et al., 2002; Braas et al., 2006) and PACAP expression in dorsal root ganglia (DRG) and afferent projections in the spinal cord are upregulated following bladder inflammation induced by cyclophosphamide (CYP) (Vizzard, 2000c) or after spinal cord injury (Zvarova et al., 2005; Zvara et al., 2006). Consistent with the direct effects of PACAP and VIP in other smooth muscle systems (Schworer et al., 1993; Steenstrup et al., 1994; Linden et al., 1999; Fizanne et al., 2004), we have previously demonstrated specific PACAP receptor expression in bladder smooth muscle, urothelium, lumbosacral DRG and spinal cord suggesting that PACAP and PAC1 receptor signaling participate at multiple levels along the lower urinary tract (LUT) (Braas et al., 2006). One goal of the present study was to characterize the regulation of PACAP and VIP and associated receptor expression in urothelium, detrusor smooth muscle, and lumbosacral DRG as a function of increasing duration of bladder inflammation induced by CYP using real-time quantitative reverse transcription-polymerase chain reaction (Q-PCR). We also examined expression of two other neuropeptides, substance P (Vizzard, 2001) and galanin (Zvarova and Vizzard, 2006), not members of the PACAP/VIP family, but expressed in LUT pathways and regulated with bladder inflammation (Vizzard, 2001; Zvarova and Vizzard, 2006).
Purinergic signaling pathways may play an important role in regulating normal urinary bladder function including detrusor smooth muscle contraction (Brown et al., 1979; King et al., 1997) and bladder filling sensation (Burnstock, 2000; Rong et al., 2002) and changes in purinergic signaling have been implicated in bladder dysfunction (Bodin and Burnstock, 1998; Sun et al., 2001a; Sun et al., 2001b; Birder et al., 2003; Birder et al., 2004). Earlier studies have indicated that the urothelium releases adenosine triphosphate (ATP) in response to various stimuli (Birder, 2006). In addition, it has been suggested that ATP released from the serosal surface of the urothelium during bladder filling stimulates P2X3 receptors on suburothelial sensory nerve fibers and contributes to bladder filling sensation (Cockayne et al., 2000). ATP in the cell cytoplasm can be released extracellularly by several mechanisms including exocytosis of ATP-containing vesicles (Bodin and Burnstock, 2001; Novak, 2003). An additional goal of this study was to determine if PACAP and VIP receptors in normal bladder urothelium are functional by measurement of PACAP and/or VIP-evoked ATP release.
Acute, intermediate and chronic CYP-induced cystitis rat models were examined in these studies (Corrow and Vizzard, 2007; Klinger et al., 2008). Chronic CYP-induced cystitis: rats received drug injection (75 mg/kg; intraperitoneal, i.p.) every third day for 8 days. Intermediate CYP-induced cystitis: rats received a single injection (150 mg/kg, i.p.) and tissues were examined 48 hours (hr) later. Acute CYP-induced cystitis: rats received a single injection (150 mg/kg, i.p.) and survived for 4 hours (hr). Control rats received volume-matched injections of saline (0.9%; i.p.) or no treatment and no difference among the control groups was observed. All injections were performed under isoflurane (2%) anesthesia. The CYP model of bladder inflammation produces an increase in voiding frequency with small micturition volumes and is associated with inflammatory cell infiltrates in the urinary bladder including mast cells, macrophages and neutrophils (Vizzard, 2000a; Hu et al., 2003; LaBerge et al., 2006). All experimental protocols involving animal use were approved by the University of Vermont Institutional Animal Care and Use Committee (IACUC # 06–014). Animal care was under the supervision of the University of Vermont's Office of Animal Care Management in accordance with the Association for Assessment and Accreditation of Laboratory Animal Care (AAALAC) and National Institutes of Health guidelines. All efforts were made to minimize the potential for animal pain, stress or distress.
After CYP treatment or in control situations (control, 4 hr, 48 hr, or chronic; n = 5 – 7 for each), animals were deeply anesthetized with isoflurane (3–4%) and then euthanized via thoracotomy. The urinary bladder and DRG were quickly removed. Whole bladder was dissected under RNase-free conditions. The bladder was cut open along the midline and pinned to a sylgard-coated dish and the urothelium was removed as previously described (Zvarova and Vizzard, 2005). The urothelium has suburothelial structures associated with it; the term urothelium in this paper refers to both urothelial and suburothelial structures. DRG were identified and isolated as previously described (Vizzard, 1997; Vizzard, 2000a; Vizzard, 2000c) under RNase-free conditions. Lumbosacral DRG (L6, S1) were specifically chosen for analysis based upon the previously determined segmental representation of urinary bladder circuitry (Donovan et al., 1983; Keast and de Groat, 1992; Nadelhaft and Vera, 1995). Bladder afferents are not distributed within the L4–L5 DRG (Donovan et al., 1983; Keast and de Groat, 1992) that contain only somatic afferents nor are neurons that are involved in urinary bladder function observed in the L4–L5 spinal segments (Nadelhaft and Vera, 1995). Harvest of DRG was restricted to L6-S1 because previous studies have demonstrated the presence of PAC1 and VPAC2 receptors in these tissues using non-quantitative reverse-transcription polymerase chain reaction (Braas et al., 2006).
Total RNA was extracted using the STAT-60 total RNA/mRNA isolation reagent (Tel-Test‘B’, Friendswood, TX, USA) as previously described (Girard et al., 2002; Klinger et al., 2008). One to 2 mg of RNA per sample was used to synthesize complementary DNA using SuperScript II reverse transcriptase and random hexamer primers with the SuperScript II Preamplification System (Invitrogen, Carlsbad, CA, USA) in a 20 µl final reaction volume.
The quantitative PCR standards for all transcripts were prepared with the amplified PAC1, VPAC1, VPAC2, PACAP, VIP, Gal, Sub P and L32 cDNA products ligated directly into pCR2.1 TOPO vector using the TOPO TA cloning kit (Invitrogen). The nucleotide sequences of the inserts were verified by automated fluorescent dideoxy dye terminator sequencing (Vermont Cancer Center DNA Analysis Facility). To estimate the relative expression of the receptor transcripts, 10-fold serial dilutions of stock plasmids were prepared as quantitative standards. The range of standard concentrations was determined empirically.
Real-time quantitative PCR was performed using SYBR Green I detection (Girard et al., 2002; Klinger et al., 2008). Complementary DNA templates, diluted 5-fold to minimize the inhibitory effects of the reverse transcription reaction components, were assayed using SYBR Green I JumpStart™. Taq ReadyMix™ (Sigma, St. Louis, MO, USA) containing 5 mM MgCl2, 200 mM dATP, dGTP, dCTP and dTTP, 0.64 U Taq DNA polymerase and 300 nM of each primer in a final 25-µl reaction volume. The real-time quantitative PCR was performed on an Applied Biosystems 7500 Fast real-time PCR system (Applied Biosystems, Foster City, CA, USA) (Girard et al., 2002; Klinger et al., 2008) using the following standard conditions: (i) 94 °C for 2 min; (ii) amplification over 40 cycles at 94 °C for 15 s and 60 to 64 °C depending on primers set for 40 s.
The amplified product from these amplification parameters was subjected to SYBR Green I melting analysis by ramping the temperature of the reaction samples from 60°C to 95°C. A single DNA melting profile was observed under these dissociation assay conditions demonstrating amplification of a single unique product free of primer dimers or other anomalous products. Oligonucleotide primer sequences for PACAP (Girard et al., 2002), VIP (Girard et al., 2002), PAC1 (Braas and May, 1999), VPAC1 (Girard et al., 2006), VPAC2 (Girard et al., 2006), substance P (Girard et al., 2002), galanin (Girard et al., 2002) and L32 (Klinger et al., 2008) used in these studies have been previously described.
For data analyses, a standard curve was constructed by amplification of serially diluted plasmids containing the target sequence. Data were analyzed at the termination of each assay using the Sequence Detection Software version 1.3.1 (Applied Biosystems, Norwalk, CT). In standard assays, default baseline settings were selected. The increase in SYBR Green I fluorescence intensity (ΔRn) was plotted as a function of cycle number and the threshold cycle was determined by the software as the amplification cycle at which the ΔRn first intersects the established baseline. All data are expressed as the relative quantity of the gene of interest normalized to the relative quantity of the housekeeping gene L32. Control samples are set equal to 100%.
Urothelial cells were cultured 18–72 hrs prior to testing as previously described (Chopra et al., 2005; Wang et al., 2005). For each urothelial culture, at least three rat bladders were required to achieve sufficient numbers of dissociated cells for the ATP release assay. For ATP release, a perfusate of 100 µl of HBSS (5 mM KCl, 0.3 mM KH2PO4, 138 mM NaCl, 4 mM NaHCO3, 0.3 mM Na2HPO4, 5.6 mM Glucose, 2 mM CaCl2, 1 mM MgCl2, and 10 mM HEPES, pH 7.4) was collected every 30 seconds. After measuring background release of ATP from the cultures for 5–10 minutes, the test compounds were applied through the perfusion system (Rainin Peristaltic Pump RP-1, Oakland, CA) for another 5–10 minutes. ATP measurements were calculated based on the luciferin-luciferase reaction using a standard curve (Adenosine Triphosphate Assay Kit, Sigma; Turner Systems luminometer TD-20/20, Sunnyvale, CA). Data were obtained from at least three independent cultures and at least n = 3 for each culture. Data were analyzed by calculating the area under the curve during each portion of the experiment and by calculating the fold increase in ATP release using the initial perfusates as 1.0-fold.
All standard chemicals were obtained from Sigma-Aldrich or Fisher and were either analytical or laboratory grade. PACAP27, PACAP38, and VIP were purchased from American Peptide Company, Sunnyvale, CA. The PAC1 selective antagonist, M65, was a gift from Dr. Ethan Lerner, Harvard Medical School.
All data are presented as mean ± S.E.M. One-way analysis of variance (ANOVA) was used to evaluate differences among groups for Q-PCR. Data obtained from the ATP release assays violated the assumptions of the ANOVA. Thus, these data were analyzed using a non-parametric analysis, the Mann-Whitney Rank Sum test. Differences were considered statistically significant if p ≤ 0.05. When F ratios exceeded the critical value (p ≤ 0.05), the Newman-Keul's post-hoc test was used to compare the experimental means.
Previous studies (Vizzard, 2000a; Hu et al., 2003) have detailed the histological examinations and myeloperoxidase (MPO) assays that were used to establish inflammation of the urinary bladder after CYP. Gross microscopic analysis of urinary bladders from animals treated chronically with CYP resulted in extensive regions of mucosal erosion, ulcerations, edema, and, in some instances, petechial hemorrhages. Histological changes evident after chronic CYP treatment included edema of the lamina propria and plasma cell infiltrates in the lamina propria, submucosa, and perivascular tissue. Inflammatory changes are evident in urinary bladder as early as 2 hr after CYP treatment and increase in severity with time and repeated dosing with CYP. Gross microscopic analyses of bladders from animals treated with CYP 4 hr or 48 hr before examination showed a few, scattered regions of mucosal erosion on the luminal surface (Hu et al., 2003). The number and distribution of mast cells and macrophages as well as MPO activity increased with the duration of CYP treatment (chronic > 48 hr > 4 hr; Hu et al., 2003). Bladder hyperreflexia is evident as early as 4 hr after CYP-treatment (Hu et al., 2003).
PAC1, VPAC1 and VPAC2 receptor transcripts were expressed in the urothelium and detrusor smooth muscle of control (non-inflamed) urinary bladder (Fig. 1A–C) as previously described (Braas et al., 2006). With acute (4 hr) CYP-induced cystitis, PAC1 receptor transcript exhibited a significant (p ≤ 0.05) decrease in expression in both urothelium and detrusor with a significant (p ≤ 0.05) increase in PAC1 receptor transcript expression in urothelium and detrusor smooth muscle induced by intermediate (48 hr) and chronic (8 d) CYP-induced cystitis (Fig. 1A). CYP-induced changes in VPAC1 and VPAC2 expression were similar in both urothelium and detrusor (Fig. 1B, C). Acute (4 hr) and intermediate (48 hr) CYP-induced cystitis increased VPAC1 and VPAC2 receptor transcript expression in both urothelium and detrusor. In contrast, chronic (8 day) CYP-induced cystitis, decreased VPAC2 receptor transcript expression in both urothelium and detrusor (Fig. 1C).
Transcripts for each of these neuropeptides were present in urothelium and detrusor of control (non-inflamed) urinary bladder but the effects of CYP-induced cystitis on each neuropeptide expression differed (Fig. 2A–D). PACAP transcript expression significantly (p ≤ 0.05) increased in the urothelium with intermediate (48 hr) and chronic (8 day) CYP-induced cystitis whereas no changes were observed with acute (4 hr) CYP-induced cystitis in either urothelium or detrusor smooth muscle (Fig. 2A). No regulation of VIP transcript expression was detected at any duration of CYP treatment in urothelium or detrusor (Fig. 2B). With respect to bladder inflammation-induced changes in galanin or substance P transcript expression, very different regulation was demonstrated (Fig. 2C, D). Acute (4hr) CYP-induced cystitis significantly (p ≤ 0.05) increased galanin transcript expression in the urothelium whereas chronic (8 day) CYP treatment significantly (p ≤ 0.05) increased substance P transcript expression in the detrusor smooth muscle (Fig. 2C, D).
PAC1, VPAC1 and VPAC2 receptor transcripts are expressed in the lumbosacral (L6-S1) DRG (Fig. 3A–C) as previously described (Braas et al., 2006). CYP-induced inflammation of the urinary bladder only affected receptor transcript expression following acute (4 hr) CYP-induced cystitis (Fig. 3A–C). PAC1 and VPAC2 receptor transcript expression significantly (p ≤ 0.05) decreased in both L6 and S1 DRG with acute (4 hr) CYP-induced cystitis (Fig. 3A, C). For VPAC1 receptor transcript expression, a significant (p ≤ 0.05) increase in expression was demonstrated in the S1 DRG after acute CYP-induced cystitis (Fig. 3B). No changes in PAC1, VPAC1 or VPAC1 receptor expression in L6 or S1 DRG were demonstrated with intermediate (48 hr) or chronic (8 day) CYP-induced cystitis (Fig. 3A–C).
In contrast to the few changes in neuropeptide transcript expression demonstrated in the urothelium and detrusor smooth muscle with CYP-induced cystitis, greater regulation was demonstrated in the L6 and S1 DRG (Fig. 4A–D). Changes in PACAP transcript with CYP-induced cystitis mirrored those observed in the urinary bladder with acute CYP-induced cystitis decreasing and intermediate (48 hr) and chronic (8 day) treatments significantly (p ≤ 0.05) increasing PACAP transcript expression in both the L6 and S1 DRG (Fig. 4A). Similar to the lack of regulation demonstrated for VIP transcript in the urinary bladder with CYP-induced cystitis, cystitis was also without effect on VIP regulation in the L6 and S1 DRG (Fig. 4B). Galanin transcript expression significantly (p ≤ 0.05) decreased in the L6 DRG following 4 hr or 8 day CYP-induced cystitis (Fig. 4C). In contrast, substance P transcript expression significantly (p ≤ 0.05) increased in the L6 DRG with intermediate (48 hr) and chronic (8 day) cystitis (Fig. 4D). Acute (4 hr) CYP treatment significantly (p ≤ 0.05) decreased substance P transcript expression in the L6 DRG (Fig. 4D).
ATP release from normal rat urothelial cell cultures was significantly (p ≤ 0.01) increased after stimulation with PACAP27 (100 nM) (Fig. 5). PACAP27 evoked release of ATP was significantly (p ≤ 0.01) inhibited by the PAC1 specific receptor antagonist, M65 (1 µM). PACAP38 (100 nM) also increased ATP release from normal rat urothelial cell cultures but release was less than that observed with PACAP38.
Pituitary adenylate cyclase activating polypeptide (PACAP) peptides have diverse functions in the endocrine, nervous, gastrointestinal and cardiovascular systems (Braas and May, 1996; Arimura, 1998) through PAC1, VPAC1 and VPAC2 G protein-coupled receptors. High levels of PACAP and vasoactive intestinal polypeptide (VIP) expression have been identified in many central nervous system neurons and in sensory and autonomic ganglia (Arimura et al., 1991; Sundler et al., 1996; Moller et al., 1997a; Moller et al., 1997b; Arimura, 1998; Braas et al., 1998). Both PACAP- and VIP-immunoreactivity have been identified in urinary bladder (Fahrenkrug and Hannibal, 1998). The majority of the PACAP nerve fibers are derived from sensory neurons (Zhang et al., 1995; Fahrenkrug and Hannibal, 1998; Zvarova et al., 2005). By contrast, bladder VIP-immunoreactive fibers exhibited distribution patterns that were distinct from PACAP and were not sensitive to capsaicin suggesting that they may be derived from pelvic autonomic ganglia (Fahrenkrug and Hannibal, 1998).
PACAP and VIP peptides regulate smooth muscle function, either directly or by facilitating cholinergic and nitric oxide mechanisms, in a tissue- and species-specific manner (Mizumoto et al., 1992; Fox-Threlkeld et al., 1999; Onaga et al., 1998; Seebeck et al., 2002; Zizzo et al., 2004). A number of studies have implicated PACAP in lower urinary tract (LUT) function (Vizzard, 2000c ; Zvarova et al., 2005; Braas et al., 2006; Herrera et al., 2006; Zvara et al., 2006). Similar to previous studies for calcitonin gene-related peptide (CGRP) and substance P (Mohammed et al., 2002), CYP-induced cystitis altered the expression of PACAP in micturition pathways. Acute and chronic CYP-treatment in rats increased PACAP staining in lumbosacral DRG neurons and central projections to corresponding spinal cord segments (Vizzard, 2000c). Recent studies also demonstrated upregulation of PACAP in LUT tissues after chronic spinal cord injury (Zvarova et al., 2005). These observations were consistent with neurophenotypic changes in DRG and spinal cord following injury and inflammation (Zhang et al., 1996; Zhang et al., 1998; Jongsma Wallin et al., 2003), and suggested that among other sensory peptides, increased PACAP expression in the micturition pathways may participate in the physiological pathologies associated with bladder inflammation. Thus, by extrapolation, we have suggested that PACAP peptides may contribute to the clinical syndrome of interstitial cystitis (IC)/painful bladder syndrome (PBS).
IC/PBS is a chronic inflammatory bladder disease syndrome characterized by urinary frequency, urgency, suprapubic and pelvic pain. Although the etiology and pathogenesis of IC are unknown, numerous theories including; infection, autoimmune disorder, toxic urinary agents, deficiency in bladder wall lining and neurogenic causes have been proposed (Erickson and Davies, 1998; Erickson, 1999; Sant and Theoharides, 1999; Rosamilia and Dwyera, 2000). CYP-administration to rats results in bladder inflammation, and reduced bladder capacity and intercontraction intervals (Maggi et al., 1992; Maggi et al., 1993; Hu et al., 2003). We have previously demonstrated that PACAP expression is upregulated in spinal cord and DRG (Vizzard, 2000c) with bladder inflammation. In the present study, we extend those findings to demonstrate that PACAP transcript expression is also increased in the urinary bladder and lumbosacral DRG with bladder inflammation. In experimental inflammation paradigms, the expression of several sensory peptides including PACAP is increased while VIP levels, by contrast are unchanged (Donaldson et al., 1992; Lu et al., 2005). Consistent with these previous studies, no changes in VIP transcript expression were observed in the urinary bladder or L6-S1 DRG after CYP-induced cystitis. The changes in PACAP transcript in the lumbosacral DRG were very similar to those observed for substance P transcript expression after CYP-induced cystitis (Vizzard, 2001). This similar regulation may reflect colocalization of PACAP and substance P in some sensory neurons. Both PACAP and substance P are expressed in bladder afferent neurons and CYP-induced cystitis increases the percentage of bladder afferent cells that express PACAP or substance P (Vizzard, 2000c; Vizzard, 2001). It would be of interest in the future to determine whether bladder afferent neurons in the DRG express both PACAP and substance P. In contrast, a small percentage of bladder afferent cells express galanin-immunoreactivity and this expression is largely unaffected by CYP-induced intermediate or chronic cystitis (Zvarova and Vizzard, 2006). This finding is consistent with the present demonstration that intermediate or chronic cystitis has no effect on galanin transcript expression in L6-S1 DRG despite a reduction in transcript expression with acute CYP-induced cystitis.
PACAP- and VIP-immunoreactive fibers have been identified in the bladder wall and suburothelial plexus, PACAP peptides have been measured in bladder tissues (Fahrenkrug and Hannibal, 1998) and we have recently identified PACAP/VIP receptor subtypes and isoforms in LUT (Braas et al., 2006). As PACAP and VIP share receptor subtypes coupled to different intracellular effectors, the identification of specific PACAP/VIP receptors can be important in revealing the relevant peptides and their signaling mechanisms in LUT physiology. Only PACAP peptides exhibit high affinity for the PAC1 receptor, whereas VIP and PACAP have similar high affinities for the VPAC1 and VPAC2 receptors (Arimura, 1998; Sherwood et al., 2000; Vaudry et al., 2000). While VPAC receptors appear to be coupled solely to adenylyl cyclase, PAC1 receptor isoforms display unique patterns of adenylyl cyclase and phospholipase C activation that differ for the alternatively processed PACAP27 and PACAP38 peptides (Spengler et al., 1993; Arimura, 1998; Sherwood et al., 2000; Vaudry et al., 2000). Although PACAP/VIP receptor subtypes were identified in LUT (Braas et al., 2006), there were still a number of deficits in our knowledge regarding PACAP/VIP receptors in the LUT including receptor regulation in LUT with bladder inflammation induced by CYP.
As demonstrated in the present study, PACAP/VIP receptors transcript expression is regulated by CYP-induced cystitis in both lumbosacral (L6-S1) dorsal root ganglia (DRG) and in the urothelium and detrusor smooth muscle. In the present studies, we focused our examination of PACAP/VIP receptor regulation to the urinary bladder (urothelium, detrusor smooth muscle) and the lumbosacral DRG. We have previously demonstrated that a large percentage of bladder afferent cells in the DRG express PACAP after CYP treatment and intravesical (i.e., intrabladder) infusion of the PACAP antagonist, PACAP6-38, reduced urinary bladder hyperreflexia after CYP-treatment (Braas et al., 2006). In agreement with the demonstration that PACAP (Vizzard, 2000c) is upregulated in spinal cord, DRG and urinary bladder after CYP-induced cystitis, the present data demonstrate that CYP-induced cystitis upregulates PAC1 receptor transcript expression in the urinary bladder at all durations of CYP-treatment. Similarly, VPAC1 and VPAC2 receptor transcripts were also increased with acute and intermediate CYP-induced cystitis; however, VPAC2 receptor transcript decreased in urinary bladder after chronic (8 day) CYP treatment.
We have previously demonstrated direct effects of PACAP on bladder smooth muscle contractility (Braas et al., 2006). Both PACAP27 and PACAP38 increased bladder smooth muscle tone and potentiated electric field stimulation (EFS)-induced contractions (Braas et al., 2006). EFS-induced contractions were superimposed on spontaneous muscle contractions and were tetrodotoxin-insensitive suggesting that the responses were direct detrusor smooth muscle effects (Braas et al., 2006). Surprisingly, VIP had no apparent effects on either bladder tone or EFS-stimulated contractions despite VPAC2 receptor transcript expression in detrusor (Braas et al., 2006). However, as VIP innervation to the urinary bladder is minimal compared to that for PACAP (Fahrenkrug and Hannibal, 1998), these results may be in keeping with suggestions that PACAP and PAC1 signaling are more prominent regulators of rat bladder physiology (Braas et al., 2006). These VIP results are consistent with previous studies that demonstrated that VIP application to detrusor smooth muscle had not effect on spontaneous or carbachol-induced bladder contractions despite facilitation of micturition when VIP was administered intrathecally or intraarterially close to the rat bladder (Igawa et al., 1993). In the present studies, PACAP27, PACAP38 and VIP application evoked ATP release from rat urothelial cell cultures; however, ATP release was greatest with PACAP27 treatment and significantly blocked by the PAC1 receptor selective antagonist, M65. The current data further support the suggestion that PACAP and PAC1 signaling are regulators of bladder physiology at the level of the urinary bladder and specifically, the urothelium.
CYP-induced cystitis alters the expression of tissue-derived growth factors and receptors including NGF, TrkA and p75NTR (Murray et al., 2004; Vizzard, 2000b; Hu et al., 2005). Enhanced target-derived NGF availability has been shown to increase PACAP expression in small nociceptive neurons in DRG (Vizzard, 2000c; Jongsma Wallin et al., 2001; Jongsma Wallin et al., 2003) that may result in increased PACAP signaling at PAC1 and/or VPAC2 receptors in peripheral tissue sites to exacerbate bladder dysfunction and sensory disturbances in cystitis (Fig. 6). As a corollary, NGF does not increase VIP expression in DRG that may be consistent with the target tissue neurotrophic model to selectively augment PACAP expression in DRG (Mulderry and Lindsay, 1990) (V. May and K. Braas, unpublished observations). Ongoing studies are designed to address LUT function in PACAP−/− mice under normal conditions and in the context of urinary bladder inflammation.
This work was funded by NIH grants DK051369, DK060481, DK065989.