- Original Articles
- Open Access
Nitric Oxide-Dependent Penile Erection in Mice Lacking Neuronal Nitric Oxide Synthase
© Molecular Medicine 1996
- Published: 1 May 1996
Nitric oxide (NO) has been implicated as a mediator of penile erection, because the neuronal isoform of NO synthase (NOS) is localized to the penile innervation and NOS inhibitors selectively block erections. NO can also be formed by two other NOS isoforms derived from distinct genes, inducible NOS (iNOS) and endothelial NOS (eNOS). To clarify the source of NO in penile function, we have examined mice with targeted deletion of the nNOS gene (nNOS− mice).
Materials and Methods
Mating behavior, electro-physiologically induced penile erection, isolated erectile tissue isometric tension, and eNOS localization by immunohistochemistry and Western blot were performed on nNOS− mice and wild-type controls.
Both intact animal penile erections and isolated erectile tissue function are maintained in nNOS mice, in agreement with demonstrated normal sexual behaviors, but is stereospecifically blocked by the NOS inhibitor, L-nitroarginine methyl ester (L-NAME). eNOS is abundantly present in endothelium of penile vasculature and sinusoidal endothelium within the corpora cavernosa, with levels that are significantly higher in nNOS− mice than in wild-type controls.
eNOS mediates NO-dependent penile erection in nNOS− animals and normal penile erection. These data clarify the role of nitric oxide in penile erection and may have implications for therapeutic agents with selective effects on NOS isoforms.
Nitric oxide (NO) participates in the tumoricidal and bactericidal actions of macrophages (1,2), accounts for endothelial-derived relaxing factor (EDRF) activity (3,4) and is a neuromodulator in the brain and peripheral nervous system (5,6). Three distinct forms of NO synthase (NOS), derived from distinct genes have been identified and are designated inducible or macrophage NOS (iNOS; NOS-2), endothelial NOS (eNOS; NOS-3), and neuronal NOS (nNOS; NOS-1) (7).
nNOS occurs in discrete neuronal populations in the brain (8) and in the peripheral autonomic nervous system where it accounts for nonadrenergic, noncholinergic (NANC) transmission in various organs (3). For example, NANC stimulation results in intestinal relaxation which appears to involve NO; intestinal relaxation is blocked by NOS inhibitors and is mediated by the myenteric plexus neurons which contain nNOS (9–12).
Penile erection involves relaxation of the smooth muscle of the corpora cavernosa by a NANC process (13,14). NO has been implicated in studies showing that NANC relaxation of penile smooth muscle is abolished by NOS inhibitors (15–20). We demonstrated nNOS staining in the pelvic plexus, the dorsal penile nerve, the cavernous nerve, and its branches in the cavernous tissue (21,22). Penile erection elicited in rats by electrical stimulation of the pelvic nerves is completely prevented by NOS inhibitors such as L-nitroarginine methyl ester (L-NAME) and by N-methyl-L-arginine but not by N-methyl-D-arginine, which does not inhibit NOS activity (21,22). Moreover, L-arginine administration restores erections, whereas D-arginine does not (21).
Recently mice with targeted disruption of nNOS have been developed (23). Gross locomotor activity, long-term potentiation in hippocampal slices (24) and long-term depression in cerebellar cultures (25) are normal in these animals. NO has been implicated in neural damage following vascular stroke, because stroke damage can be prevented with NOS inhibitors (5) and nNOS− mice are resistant to stroke damage (26). Breeding activity of nNOS− animals is superficially normal. If nNOS were fully responsible for penile erection, one might expect male mice to be impotent unless compensatory mechanisms occur. In the present study, we explore mating behavior as well as electrically induced penile erection. nNOS− mice display normal mating behavior and normal penile erection which is blocked by NOS inhibitors. We demonstrate a loss of nNOS from penile tissue of the nNOS− animals but describe a prominent eNOS system in penile tissue.
Adult male C57 BL6 and Agouti 129 (wild-type) and transgenic (nNOS−) mice were individually placed in a clear aquarium (38.5 × 26.5 × 30.7 cm), with subjacent angled observational mirrors. Following a 15-min acclimation period, an estrous wild-type female was introduced into the mating arena. Mating behavior was recorded during a 30-min observation period by two independent observers who were unaware of the animals’ genotype. Males were also paired with female C57 BL6 mice that were in natural estrus to assess fertility. Thus, behaviors (number of mounts, intromissions, and ejaculations) and fertility (number of pups sired) were recorded.
A mount was operationally defined as the male assuming the copulatory position, but failing to achieve intromission. Intromission was defined as the male’s erect penis entering the vagina in association with thrusting behavior. Ejaculation was defined by the culmination of vigorous thrusting behavior and the male’s arching his spine and lifting his forepaws off the female prior to penile withdrawal. Ejaculation was verified by the presence of a sperm plug followed by a refractory period of ≥5 min before the next mounting.
Stimulus females were ovariectomized and received subcutaneous placements of estradiol Silastic capsules. Mating tests commenced after a 2-week recuperation period. Six hours prior to the mating tests, the females were injected with 1 mg of progesterone (suspended in sesame seed oil) to induce behavioral estrus. Mating tests began 8 hr later at the onset of the dark period. Males participated in two separate mating tests, separated by 1 week.
Physiologic Erection Studies
Penile erections were electrically induced in intact adult male C57 BL6 and Agouti 129 (wild-type) and transgenic (nNOS−) mice following intraperitoneal pentobarbital anesthesia (50 mg/kg), as previously described in rats (21). Briefly, cavernous nerves arising from the ispilateral pelvic ganglion situated dorsal to the prostate were stimulated with unilaterally attached bipolar silver wire electrodes using a Grass S48 square wave stimulator at optimal parameters (2 V, 5 msec, 16 Hz, 60 sec in duration). Neurostimulated erections were visually assessed and recorded at baseline and 10 min following the intracavernous administration of arginine derivatives (nitro-L-arginine methyl ester, nitro-D-arginine methyl ester, 20 mg/kg).
Isometric Tension Studies
Isolated strips of corpus cavernosum (approximately 2 × 2 × 8 mm) were excised from penes of adult male mice C57 BL 6 and Agouti 129 (wild-type) and transgenic (nNOS−) mice following CO2 inhalation. Strips were suspended in 0.2-ml tissue chambers between two parallel platinum electrodes and bathed in Krebs physiologic salt solution (millimolar composition: NaCl 137, KCl 5.9, MgCl2 1.2, CaCl2 2.5, NaHCO3 15.5, KH2PO4 1.2, glucose 11.5) with a mixture of 95% O2 and 5% CO2, pH 7.2, at 37°C. The tissue was initially equilibrated and treated with 120 mM Krebs solution (prepared by substituting 120 mM of sodium with equimolar amounts of potassium) prior to achieving optimal resting isometric tension. Each strip was then precontracted with a supramaximal concentration of norepinephrine (10 mM). Thereafter, each strip was subjected to electrical field stimulation (10 V, 1 msec, 10-sec trains at 20, 40, 60 Hz) using a Grass S48 square wave stimulator at baseline and after sequential 15 min incubations with 1 µM nitro-L-arginine methyl ester and 1 mM L-arginine. Tension was monitored by polygraph (Gould SC286, Gould Electronics, Valley View, OH, U.S.A.). Tissue responses to chemical agents were quantified as percentages of the norepi-nephrine-induced tension.
Whole penes were removed from adult male C57 BL6 and Agouti 129 (wild-type) and transgenic (nNOS−) mice and Sprague-Dawley rats following CO2 inhalation. Specimens were homogenized in ice-cold buffer (50 mM Tris HCl, pH 7.4/1 mM EDTA/1 mM EGTA containing aprotinin [2 mg/ml], leupeptin [5 mg/ml], and pefabloc [1 mM]) and centrifuged at 10,000 × g for 1 hr. Supernatants were analyzed for total protein (Coomassie protein assay reagent, Pierce, Rockford, IL, U.S.A.) and subjected to 7.5% SDS/PAGE, transferred to Amersham Hybond-ECl nitrocellulose (Amersham, Arlington Heights, IL, U.S.A.) on a Millipore Milliblot semidry transfer system (Millipore, Marlborough, MA, U.S.A.) and probed overnight with a commercially available affinity-purified rabbit polyclonal antibody (1:250 dilution) against amino acids 1030–1209 of human eNOS (Transduction Laboratories). Blots were washed, developed by enhanced chemiluminescence (Amersham), and exposed to Kodak XAR film. To verify eNOS localizations, human endothelial lysate (Transduction Laboratories, Lexington, KY, U.S.A.) was used as a positive control. For preabsorption experiments, the antibody was preincubated with 50-fold excess bovine eNOS peptide based on amino acids 1185–1205 at 4°C for 24 hr. Intensities of the protein bands visualized roentgenographically were then measured using computer-assisted image analysis with comparisons made among samples run at identical exposures. eNOS protein was then quantified from homogenate supernatants using standard protein curves generated for each experiment from serial dilutions of human endothelial lysate in Laemmli buffer.
In separate experiments to verify the absence of nNOS immunoreactivity in nNOS− mice penes, blotting was performed using an affinity-purified rabbit polyclonal antibody (1:500 dilution) against a fusion protein corresponding to amino acids 1–181 of rat nNOS (27). To evaluate iNOS immunoreactivity in nNOS− mice penes, blotting was performed using an affinity-purified rabbit polyclonal antibody (1:5000 dilution) against the 15 amino acid carboxy terminus of murine inducible NOS (gift from Dr. Charles Lowenstein, Johns Hopkins University) with murine macrophage lysate as a positive control.
Whole penes were removed from adult male C57 BL6 and Agouti 129 (wild-type) and transgenic (nNOS−) mice and Sprague-Dawley rats following CO2 inhalation. Specimens were divided into proximal and distal segments and quickly frozen. Transverse sections (6-µm-thick) were cut on a cryostat (−18°C) and mounted onto gelatin/chrome alum-coated slides. Slide-mounted tissue sections were initially incubated in 4% freshly depolymerized paraformaldehyde in 0.1 M phosphate-buffered saline (PBS), pH 7.4, for 5 min and then permeabilized in 0.4% Triton X-100 for 15 min. All slides were subsequently incubated in PBS containing 1% (v/v) normal goat serum for 20 min and then in PBS containing a commercially available affinity-purified rabbit polyclonal antibody, either anti-eNOS antibody (1:50 dilution) against amino acids 1030–1209 of human eNOS (Transduction Laboratories) or anti-eNOS antibody (1:250 dilution) against amino acids 599–613 of bovine eNOS (Biomol Laboratories, Plymouth Meeting, PA, U.S.A.) for 1 hr at room temperature. Staining was visualized with an avidin-biotin-peroxidase system (Vector Laboratories, Burlingame, CA, U.S.A.) with diaminobenzidine as the chromogen. For controls, specimens were incubated with anti-eNOS antibody inactivated with serial dilutions of excess bovine eNOS peptide based on amino acids 1185–1205 at 4°C for 24 hr. As additional controls, specimens were processed in the absence of primary antibody. To verify endothelial staining. Factor 8 immunohistochemistry was also performed using anti-human von Willebrand factor antibody (1:200 dilution) (Sigma Chemical Co., St. Louis, MO, U.S.A.). The grade of eNOS immunohistochemical staining was compared between sections from wild-type and nNOS− mice prepared on the same slide by two independent observers.
In separate experiments to verify the absence of nNOS localizations in nNOS− mice penes, immunohistochemistry was performed using an affinity-purified rabbit polyclonal antibody (1:500) dilution against a fusion protein corresponding to amino acids 1–181 of rat nNOS (27). To confirm NOS localizations, NADPH diaphorase histochemistry was performed by incubating slide-mounted, fixed sections with 1 mM NADPH and 0.2 mM nitroblue tetrazolium in 50 mM Tris (pH 7.4) and 12% (v/v) dimethylsulfoxide for 30 min at room temperature.
Where appropriate, results are expressed as mean values ± standard error of the mean (SEM). Variables were evaluated by analysis of variance except for eNOS protein quantitations, which were analyzed as pairs between groups using the Wilcoxon signed rank test. Statistical differences were determined using Student’s t test.
Mating Behavior and NO-Dependent Penile Erection Are Normal in nNOS− Mice
Mating Test Observations*
Behavior (per 30 min. test)
Wild Type (n = 10)
nNOS-(n = 10)
Number of mounts
Number of intromissions
Number of ejaculations
Wild Type (n = 10)
nNOS-(n = 10)
Number of pups sired
Neurostimulated Penile Erections
Demonstration of eNOS in Penile Tissue
To compare eNOS staining in wild-type and nNOS− animals, two independent observers blindly evaluated nine distinct sections each from wild-type and nNOS− mice. In seven out of the nine paired comparisons of nNOS− and wild-type sections, eNOS staining was more prominent in nNOS− than wild-type animals.
The preservation of NO-dependent penile erection in nNOS− animals suggests the involvement of eNOS. Penile erections in nNOS− animals are blocked stereospecifically by the nonspecific NOS inhibitor NAME. Moreover, L-NAME augments contractile responses of corpora cavernosa muscle and L-arginine reverses this effect in nNOS− as well as wild-type animals.
The source of NO mediating penile erection in nNOS− animals does not appear to be iNOS, as we were unable to demonstrate its presence in penile tissue. By contrast, both Western blot and immunohistochemistry revealed abundant eNOS in penile tissue. There appears to be a consistent 20% increase in eNOS in nNOS− penile tissue compared with wild-type tissue. eNOS has previously been suggested to play a role in relaxation of penile smooth muscle (16,18). Acetylcholine-induced relaxation of this muscle is reversed by NOS inhibitors (16,18). NO donors relax penile smooth muscle (15). Moreover, eNOS localizations are consistent with a role in mediating relaxation of smooth muscle of the cavernosal sinusoids which is the fundamental process responsible for penile erection. It is well established that dilatation of penile arteries as well as the sinusoids is critical for erection, and eNOS occurs at both loci. Since penile erections occur in response to activation of the penile nerves, it would be important for nerve processes to release acetylcholine in the vicinity of the cell layers that contain eNOS. Neurons staining for choline acetyltransferase extend branches throughout the cavernosal tissue including the area of the endothelium (32,33).
Thus, eNOS can account for NO-dependent penile erection in nNOS− animals. It is unclear whether nNOS or eNOS is primarily responsible for erection in wild-type animals. NOS inhibitors that have been employed do not differentiate between these two forms of the enzyme. The augmented eNOS activity in the nNOS− animals presumably represents a compensatory mechanism, which might suggest that nNOS is principally involved in penile erection of wild-type animals. In support of this notion, removal of endothelial tissue does not affect NO-dependent relaxation of penile smooth muscle elicited by electrical stimulation (16).
In many instances of mice with targeted disruption of genes, compensatory mechanisms preserve the functions thought to be associated with proteins derived from the deviated genes. For example, cerebral vasodilatation induced by CO2 exposure is NO dependent, being abolished stereospecifically by NOS inhibitors and restored by L-arginine (34). The CO2 vasodilatation persists in nNOS− animals (35), but is no longer reversed by NOS inhibitors, implying compensation by some non-NO mechanism. The apparent maintenance of penile erection by eNOS in nNOS− animals may represent a unique instance in which compensation involves the same mediator derived from a separate gene.
This work was supported by a New Investigator Grant from the American Foundation for Urologic Disease with funds contributed by G. D. Searle (ALB); USPHS Grants HD22201 and CA58618 (RJN); USPHS Grant DA-00266 and Research Scientist Award DA-0074 (SHS), USPHS CIDA NS-01578 and NS33277, the Paul Beeson Physician Scholars in Aging Research Program, and the International Life Sciences Institute (TMD); and USPHS Grant NS33142 (VLD).
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