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REVIEW ARTICLE
Year : 2022 | Volume
: 33
| Issue : 3 | Page : 101-113
Current knowledge and novel frontiers in lower urinary tract dysfunction after spinal cord injury: Basic research perspectives
Naoki Wada1, Sergei Karnup2, Katsumi Kadekawa3, Nobutaka Shimizu3, Joonbeom Kwon3, Takahiro Shimizu3, Daisuke Gotoh3, Hidehiro Kakizaki4, William C de Groat2, Naoki Yoshimura5
1 Department of Urology, University of Pittsburgh School of Medicine, Pittsburgh, PA, USA; Department of Renal and Urologic Surgery, Asahikawa Medical University, Asahikawa, Japan
2 Department of Pharmacology and Chemical Biology, University of Pittsburgh School of Medicine, Pittsburgh, PA, USA
3 Department of Urology, University of Pittsburgh School of Medicine, Pittsburgh, PA, USA
4 Department of Renal and Urologic Surgery, Asahikawa Medical University, Asahikawa, Japan
5 Department of Urology; Department of Pharmacology and Chemical Biology, University of Pittsburgh School of Medicine, Pittsburgh, PA, USA
Correspondence Address:
Naoki Wada
Department of Urology, University of Pittsburgh School of Medicine, Suite 700, Kaufmann Medical Bldg, 3471 Fifth Ave, Pittsburgh, PA 15213
Source of Support: None, Conflict of Interest: None
DOI: 10.4103/UROS.UROS_31_22
This review article aims to summarize the recent advancement in basic research on lower urinary tract dysfunction (LUTD) following spinal cord injury (SCI) above the sacral level. We particularly focused on the neurophysiologic mechanisms controlling the lower urinary tract (LUT) function and the SCI-induced changes in micturition control in animal models of SCI. The LUT has two main functions, the storage and voiding of urine, that are regulated by a complex neural control system. This neural system coordinates the activity of two functional units in the LUT: the urinary bladder and an outlet including bladder neck, urethra, and striated muscles of the pelvic floor. During the storage phase, the outlet is closed and the bladder is quiescent to maintain a low intravesical pressure and continence, and during the voiding phase, the outlet relaxes and the bladder contracts to promote efficient release of urine. SCI impairs voluntary control of voiding as well as the normal reflex pathways that coordinate bladder and sphincter function. Following SCI, the bladder is initially areflexic but then becomes hyperreflexic due to the emergence of a spinal micturition reflex pathway. However, the bladder does not empty efficiently because coordination between the bladder and urethral sphincter is lost. In animal models of SCI, hyperexcitability of silent C-fiber bladder afferents is a major pathophysiological basis of neurogenic LUTD, especially detrusor overactivity. Reflex plasticity is associated with changes in the properties of neuropeptides, neurotrophic factors, or chemical receptors of afferent neurons. Not only C-fiber but also Aδ-fiber could be involved in the emergence of neurogenic LUTD such as detrusor sphincter dyssynergia following SCI. Animal research using disease models helps us to detect the different contributing factors for LUTD due to SCI and to find potential targets for new treatments.
Keywords: Brain-derived neurotrophic factor, detrusor overactivity, detrusor-sphincter dyssynergia, lower urinary tract, nerve growth factor, spinal cord
The lower urinary tract (LUT) stores and periodically releases urine. These functions depend on neural circuits located in the brain, spinal cord, and peripheral ganglia.[1],[2] Spinal cord injury (SCI) rostral to the lumbosacral level eliminates voluntary and supraspinal control of voiding, inducing initially an areflexic bladder leading to urinary retention. Later, neurogenic detrusor overactivity (DO) develops along with loss of detrusor and urethral sphincter coordination (termed detrusor sphincter dyssynergia or DSD) resulting in inefficient voiding, bladder hypertrophy, and high intravesical pressure. The recovery of reflex bladder activity after SCI is dependent on the reorganization of reflex pathways in the spinal cord and alterations in the properties of bladder afferent neurons.[3],[4] Hence, the clinical management of SCI patients should focus on LUT dysfunction (LUTD) during the storage phase (DO and LUTD) and the voiding phase (DSD and inefficient voiding). Previous studies including ours have attempted to elucidate the neurologic mechanisms crucial for the diagnosis and treatment of LUTD after SCI using SCI animal models. In this article, we focus on the neurophysiologic mechanisms involved in the control of LUT function and the changes in micturition control induced after SCI above the sacral level. We have also summarized the latest basic research studies identifying targets for treating LUTD following SCI using animal models.
Neurophysiology of the Lower Urinary TractBladder
The LUT consists of the bladder and the urethra that store and eliminates urine, respectively. These structures are regulated by three sets of peripheral nerves: sacral parasympathetic (pelvic), thoracolumbar sympathetic (hypogastric and sympathetic chain), and somatic (pudendal) nerves distributed bilaterally,[2],[5] which consist of efferent and afferent axons originating at thoracolumbar and sacral spinal levels.[4] As the bladder fills during the storage phase, the detrusor remains quiescent with minor changes in intravesical pressure. The neural pathways stimulating the bladder for micturition are quiescent during this phase because of the active inhibitory pathways.[2],[6],[7]
Although traditionally considered a passive barrier, the bladder urothelium also has specialized sensory and signaling properties that make it responsive to chemical and mechanical stimuli and engage in reciprocal chemical communication with neighboring nerves or myofibroblasts in the underlying lamina propria, which in combination with the urothelial layer comprises the bladder mucosa.[8],[9],[10] The urothelium exhibits many properties including the following: (1) expression of acetylcholine (ACh), norepinephrine (NE), tachykinins, and agonists for transient receptor potential (TRP) channels (TRPV1, TRPV4, TRPM8 receptors); (2) close physical association with afferent nerves; and (3) ability to release chemical mediators, such as adenosine triphosphate (ATP), ACh,[4] nerve growth factor (NGF), and nitric oxide (NO),[11],[12],[13] that can regulate the activity of adjacent nerves or myofibroblasts and thereby influence reflex bladder contractions.[9],[14]
External urethral sphincter
External urethral sphincter (EUS)-electromyogram (EMG) recordings are widely used for evaluating urethral function. In various species including humans, the EUS contracts (active EUS-EMG phase) to maintain urinary continence during the storage phase and relaxes (inactive EUS-EMG phase) to allow urine flow through the urethra during the voiding phase [Figure 1]. However, in some species, such as healthy rats or dogs, EUS-EMG recordings exhibit tonic activity before the onset of voiding and bursting activity during voiding [Figure 2]. This phenomenon is characterized by clusters of high-frequency spikes (active periods) separated by low-tonic activity (silent periods [SPs]), producing a pumping action (rhythmic contractions and relaxations of EUS), which is seen as intravesical pressure oscillations during cystometrograms (CMGs).[2],[15],[16],[17],[18],[19] The EUS bursting activity and pressure oscillations in CMGs are abolished by a neuromuscular blocker (bungarotoxin) or pudendal nerve transection in rats, suggesting that the EUS-pumping activity is important for efficient bladder emptying.[17],[20] Furthermore, recent studies in rats demonstrated that coordination of EUS activity and bladder during voiding is dependent on neurons in the L3/L4 spinal cord, and this L3/L4 EUS-related circuitry consists of at least two neuronal populations: segmental interneurons and propriospinal neurons projecting to the L6/S1 spinal cord, where the major output signals carried through the pudendal nerve from the Onuf's nucleus to EUS originate.[21],[22],[23],[24] Contrastingly, the EUS-pumping activity during voiding does not occur in humans, and only a minority of healthy female mice exhibit EUS bursting activity with little impact on voiding efficiency [Figure 2].[19]
Figure 1: Representative CMG and EUS-EMG recording in human. (a) CMG and EUS-EMG recordings under the normal condition show that synergic urethral relaxation (inactive EUS-EMG) occurs when voluntary bladder contraction is induced. (b) CMG and EUS-EMG after spinal cord injury show uninhibited bladder contractions (DO and DSD). CMG: Cystometrogram, EUS: External urethral sphincter, EMG: Electromyogram, DO: Detrusor overactivity, DSD: Detrusor-sphincter dyssynergia
Figure 2: Representative recordings of simultaneous measurement of CMG and EUS- EMG activity in spinal intact unanesthetized rodents. Traces A2-4, B2-4, and C2-3 depict sections of traces A1, B1, and C1, respectively, on expanded time scales. A1-A4 show the IVP and EUS-EMG recordings during a continuous infusion CMG in a spinal intact rat. The EUS-EMG exhibits tonic activity before the onset of voiding and bursting activity during voiding (A2-4). The EUS bursting is characterized by clusters of high-frequency spikes (APs) separated by low tonic activity (SPs) (A3 and A4). The bursting produces rhythmic contractions and relaxations of the EUS and is thought to generate a urethral pumping action during voiding, which is seen as pressure oscillations on the continuous CMG tracing (A4). B1-B4 and C1-C4 show the IVP and EUS-EMG recordings during a continuous infusion CMG in a spinal intact mouse without pressure oscillation (B1–B4), and in a spinal intact mouse with pressure oscillation (C1–C4). Some mice exhibit reduced EUS activity without bursting and no obvious pressure oscillation during voiding (B1–B4). The other mice exhibit bursting-like EUS activity during voiding bladder contractions, similar to EUS busting in spinal intact rats (C1–C4), consisting of APs, and reduced EMG activity (SPs), which coincide with IVP oscillations in the CMG tracing, but the IVP oscillations in the CMG tracing were less obvious compared with those in spinal intact rats. (Modified from Kadekawa et al., 2016[19]). CMG: Cystometrogram, EUS: External urethral sphincter, EMG: Electromyogram, IVP: intravesical pressure, Aps: Active periods, SPs: Silent periods, Aps: Alternating tonicsEfferent nerves
The LUT efferent pathways are innervated by parasympathetic, sympathetic, and somatic nerves with the parasympathetic pathway providing the major excitatory input to the bladder.[2],[7] Cholinergic parasympathetic preganglionic neurons located in the intermediolateral region of the sacral spinal cord send axons through the pelvic nerves to the ganglion cells in the pelvic plexus and the bladder wall.[5] Parasympathetic postganglionic nerves excite the bladder smooth muscles by releasing cholinergic (ACh) and nonadrenergic, noncholinergic transmitters (ATP) that act on muscarinic cholinoceptors and P2X1 purinoceptors, respectively.[5] Postganglionic axons continue for a short distance in the pelvic nerve and terminate in the detrusor layer, where they release ACh to induce contractions of the detrusor smooth muscle fibers. Muscarinic inhibitory and facilitatory receptors are also present on parasympathetic nerve terminals.[25] Along with parasympathetic stimulation of bladder smooth muscles, some postsynaptic parasympathetic neurons cause relaxation of the urethral smooth muscle, possibly through NO release.[26],[27],[28]
Sympathetic pathways to the LUT, originating in the lumbar spinal cord, elicit various effects, including the following: (1) inhibition of the detrusor muscle through β-adrenoceptors and (2) excitation of the bladder neck and urethra through α1-adrenoceptors.[2],[5] Preganglionic sympathetic neurons are located in the intermediolateral column of thoracolumbar cord segments T11 to L2 in humans and[26] most preganglionic fibers synapse with postganglionic neurons in the inferior mesenteric ganglia. The preganglionic neurotransmitter, ACh, acts through nicotinic receptors in the postganglionic neurons whose axons travel in the hypogastric nerve and release NE at their terminals. Somatic nerves provide excitatory innervation to the striated muscles of the EUS and pelvic floor. The efferent motoneurons are in the Onuf's nucleus, along the lateral border of the ventral horn in sacral spinal cord segments S2 to S4 in humans.[29] Motoneuron axons are present in the pudendal nerve and release ACh at their terminals, which acts on nicotinic receptors in the striated muscle, inducing muscle contraction to maintain EUS closure.
Afferent nerves
Afferent fibers of the pelvic, hypogastric, and pudendal nerves carry sensory information from the LUT to the lumbosacral region.[2],[4],[30] The afferents passing from the pelvic nerve to the sacral spinal cord are important for initiating micturition. Light and electron microscopy studies have revealed that the visceral nerves innervating the LUT are composed primarily of small myelinated (Aδ-fiber) and unmyelinated (C-fiber) axons.[31],[32] Dorsal root ganglion (DRG) neurons give rise to myelinated Aδ- and unmyelinated C-fiber axons, which are distinguishable through immunohistochemical staining for a 200 kDa neurofilament (NF) protein that is exclusively expressed in the myelinated Aδ-fiber DRG neurons.[33] Approximately two-thirds of the bladder afferent neurons identified in rats using axonal tracing methods are NF-poor (i.e., C-fiber neurons), which are sensitive to capsaicin. The remaining neurons exhibit intense NF immunoreactivity (Aδ-fiber neurons).[34] These afferents, including small myelinated (Aδ) and unmyelinated (C) fibers, convey information from receptors in the bladder wall to second-order neurons in the spinal cord. In cats, the Aδ bladder afferents respond in a graded manner to passive distension and active contraction of the bladder, whereas the unmyelinated C-fiber ones are insensitive to mechanical stimuli and do not respond to even high levels of intravesical pressure.[4],[35] Silent C-fiber afferents have a specialized function, such as signaling during inflammatory or noxious events in the LUT.
Changes in Micturition Control Induced After Spinal Cord InjuryChanges in the bladder
In animals and humans with suprasacral lesions, CMGs exhibit intrinsic and reflex contractions (i.e., neurogenic DO) during bladder filling that are absent in individuals with intact spinal cords.[1],[3],[36] In addition, maximal voiding pressure is increased, voiding efficiency is reduced, and the bladder undergoes marked hypertrophy.[15],[16],[37] Recordings of contractile activity of in vitro whole bladders or bladder strips from SCI animals reveal large-amplitude phasic contractions similar to those seen in adult bladders with partial outlet obstruction.[38],[39],[40],[41],[42]
The bladder urothelium is also altered after SCI in rodents. In rats, within 2 h after spinal transection, the umbrella cell layer continuity is disrupted, and the transepithelial resistance (TER) is markedly reduced.[43] Twenty-four hours after SCI, TER reaches a minimum, and water and urea permeability are significantly increased. Although these changes are reversed within 2 weeks, they can be prevented by treatment with a ganglionic blocking agent, indicating that they are mediated by activity in autonomic nerves. Long-term changes include increased the expression of gap junction proteins: connexin 26 in the urothelium and connexin 43 in the lamina propria in rat bladders,[38] altering bladder function after SCI. Optical imaging techniques have revealed that phasic contractions in SCI mice bladders originate from localized sites in the bladder dome and are driven by activity arising in the urothelium.[44] Removal of the mucosa eliminated these contractions in SCI rat bladders.[39] In addition, gap junction blockers suppress phasic contractions.[38] On the basis of this, it was proposed that phasic activity in bladders after SCI might be due to signaling pathways originating in the urothelium and then passing through gap junctions through the myofibroblast network in the lamina propria to smooth muscles and afferent nerves.[39]
Changes in the external urethral sphincter
Although DO during urine storage is similar in both rats and mice after SCI,[44],[45] the behavior of the EUS during voiding is different in these two species.[19] In SCI rats, EUS bursting occurs during voiding bladder contractions, coinciding with small amplitude intravesical pressure oscillations during cystometry [Figure 3]. Nevertheless, instead of clear EUS bursting or intravesical pressure oscillation, SCI mice exhibit intermittent voiding with slow, large amplitude reductions in intravesical pressure, occurring during periods of reduced EUS activity [Figure 3].[19] α-bungarotoxin improves voiding by reducing urethral outlet resistance in SCI rats.[20] However, in healthy rats, it reduces voiding efficiency by suppressing high-frequency phasic sphincter activity necessary for efficient urine elimination in spinal intact conditions. Although the reflex EUS-pumping activity recovers and promotes voiding in rats after SCI, it is not seen in female mice.[19] This might be because of the difference in urethral activity during the voiding phase in these two species. Bilateral transection of the hypogastric nerves, which provide the major sympathetic input to the urinary bladder and proximal urethra, improves voiding in SCI rats, suggesting that abnormal sympathetic reflexes are also involved in LUTD after SCI.[46] In this article, we focus on SCI-induced DSD resulting in inefficient voiding, which is the major urethral dysfunction after SCI. Previous studies have shown that α-adrenoceptor blockers effectively improved SCI-induced inefficient voiding by reducing urethral pressure in rats,[47],[48] although they suggested that their effects are mediated by changes in EUS function or improvement of bladder ischemia. Nevertheless, the functional changes in the internal urethral sphincter comprising smooth muscles after SCI must be further explored.
Figure 3: Representative recordings of simultaneous measurement of CMG and EUS- EMG activity in a SCI rat (A1–A4) and an SCI mouse (B1–B4). Traces A2–A4 and B2–B4 are expanded from the traces A1 and B1, respectively, with different time scales. The SCI rat (A1–A4) exhibited EUS bursting with alternating APs and SPs during voiding bladder contractions, which coincided with rapid pressure oscillations in the CMG tracing. The SCI mouse (B1–B4) had intermittent voiding coinciding with more prolonged reductions in intravesical pressure in the CMG recording, which occurred during periods of low-tonic, synergic EUS-EMG activity (B3 and B4). Clear EUS bursting activity or intravesical pressure oscillations were not seen in the SCI mouse. #symbols in B3 and B4 indicate the reduced EUS activity (R-EA) during voiding.(Modified from Kadekawa et al., 2016[19]). CMG: Cystometrogram, EUS: External urethral sphincter, EMG: Electromyogram, SCI: Spinal cord-injuredChanges in bladder reflexes
Studies show that C-fiber bladder afferents, which usually do not respond to bladder distention (i.e., silent C-fibers), become mechanosensitive and initiate automatic micturition after SCI.[35] In SCI cats, micturition is induced by C-fiber afferent pathways. In chronic spinalized cats, desensitization of TRPV1-expressing C-fiber afferent pathways by subcutaneous administration of capsaicin, a C-fiber neurotoxin that binds to TRPV1 receptors, can significantly block DO during the storage phase, whereas this inhibitory effect is not seen on reflex bladder contractions in spinal intact cats.[49],[50] In SCI rats, both Aδ and C-fiber afferents can evoke bladder reflexes[36] and increased excitability of the latter induces DO because desensitizing C-fiber afferents using systemic capsaicin administration substantially suppressed nonvoiding bladder contractions without affecting the voiding reflex.[51] These results indicate that C-fiber afferents are necessary for generating neurogenic DO during the storage phase, whereas Aδ afferents still initiate voiding in SCI rats.
Capsaicin-sensitive C-fiber bladder afferent pathways, which become hyperexcitable after SCI, are involved in the control of bladder activity in both spinal intact and SCI mice. In these mice, DO is significantly but partially dependent on capsaicin-sensitive C-fiber afferents in contrast to SCI rats,[52] in which DO is induced predominantly by capsaicin-sensitive C-fiber afferents.[51] Thus, mice and rats seem to have different C-fiber-dependent afferent mechanisms controlling bladder function.
In humans with neurogenic DO, intravesical administration of C-fiber neurotoxins (capsaicin or resiniferatoxin) symptomatically improves and reduces the density of TRPV1 and P2X3 immunoreactive nerve fibers and urothelial TRPV1 immunoreactivity.[1],[53],[54] Randomized controlled trials with SCI patients revealed that these neurotoxins effectively improved both urodynamic and clinical parameters.[1] Injecting botulinum neurotoxin type A, an agent that blocks neurotransmitter release from urothelial cells and from afferent and efferent nerves, into the bladder wall also reduces neurogenic DO and reduces the density of TRPV1- and P2X3-immunoreactive nerves.[55] These findings suggest that abnormal C-fiber afferent innervation contributes to neurogenic DO in SCI humans.
Plasticity of Neurotransmitter MechanismsNeurokinins
Destruction of lumbosacral spinal neurons expressing neurokinin-1 receptors (NK-1R) using an NK-1 ligand conjugated with saporin does not affect the voiding reflex in rats with intact spinal cords but reduces the bladder irritant effects of intravesical capsaicin and reduces nonvoiding contractions in SCI rats.[56],[57] Similarly, intrathecal administration of a selective NK-1R antagonist does not affect the micturition reflex in spinal intact rats but blocks it in SCI rats.[58] These data, coupled with the increased substance P expression in the sacral parasympathetic nucleus region in SCI rats, indicate that NK-1R activation is involved in micturition in paraplegic animals.[58]
NK-2R agonists act as bladder prokinetic agents and induce smooth muscle contractions by stimulating NK-2R in smooth muscle cells.[59],[60],[61] NK-2R agonists can produce rapid-onset and short-duration, dose-dependent elevations in bladder pressure.[62],[63],[64] In conscious, spinal intact dogs, NK-2R agonists elicit efficient voiding within minutes of the administration.[64] This effect is also observed in anesthetized, acute SCI rats.[62] Chronic administration of NK-2R agonists produces consistent and efficient voiding in SCI rats.[65] Thus, NK receptors might act as therapeutic targets for the treatment of SCI-related LUT dysfunction.
Gamma-aminobutyric acid
In the central nervous system, glutamate is a major excitatory amino acid, whereas glycine and gamma-aminobutyric acid (GABA) are major inhibitory neurotransmitters that inhibit the micturition reflex at supraspinal and/or spinal sites with additive or synergistic inhibitory effects on bladder activity.[66] Intrathecal, intravenous, or dietary glycine inhibits both bladder and urethral activity in normal and SCI rats.[67],[68] Hypofunction of glycinergic or GABAergic mechanisms in the lumbosacral spinal cord induces LUTD, such as DO or DSD, in SCI rats.[18],[67],[69] Furthermore, intrathecal muscimol and baclofen (GABAA and GABAB agonists, respectively) inhibit nonvoiding bladder contractions by suppressing C-fiber bladder afferents and improve DSD in SCI rats.[18],[69] Reduced GABAergic inhibition might contribute to the development of neurogenic DO because mRNA levels of glutamic acid decarboxylase (GAD), an enzyme involved in GABA synthesis, are decreased in the spinal cord after SCI.[69] Gene delivery of GAD using nonreplicating herpes simplex virus (HSV) vectors inhibits DO or DSD without affecting the voiding contraction in SCI rats.[70],[71]
Role of neurotrophic factors
Nerve growth factor
Neurotrophic factors including NGF, brain-derived neurotrophic factor (BDNF), NT-3, and NT-4 are important in various types of neural plasticity including the emergence of LUTD in SCI.[13],[72],[73],[74] NGF is a well-researched neurotrophin that regulates the developing nervous system. DSD-induced overdistention of the bladder and decreased voiding efficiency after SCI increases NGF production in the bladder that might enhance C-fiber afferent nerve excitability, leading to neurogenic DO [Figure 4][73],[75],[76],[77] because capsaicin treatment inhibits bladder overactivity without affecting voiding contractions in SCI rats and mice.[36],[51],[52] Both neutralization of NGF and desensitization of C-fiber afferents with capsaicin or resiniferatoxin similarly suppress bladder overactivity in SCI rats and mice.[52],[75],[77],[78] NGF production is increased not only in the bladder but also in the lumbosacral spinal cord and in DRG.[77],[79] Overdistension of the bladder might stimulate an increase in NGF levels because its levels also increase in the bladder of rats after partial obstruction of the urethral outlet or in the urine of humans with bladder outlet obstruction.[80],[81] Reports have shown that NGF produced in the bladder is transported to DRG cell bodies and their spinal projections.[13] Intravesical administration of NGF in rats acutely increases reflex bladder activity, and chronic administration into the spinal cord or the bladder wall of rats induces bladder hyperactivity and increases the firing frequency of dissociated bladder afferent neurons.[73],[79],[82],[83]
Figure 4: Diagram showing hypothetical mechanisms underlying storage and voiding dysfunction induced by increasing expression of neurotrophic factors following SCI. Injury to the spinal cord causes DSD, leading to functional urethral obstruction, reduced voiding efficiency, urinary retention and bladder hypertrophy, resulting in increased levels of NGF in the bladder. NGF is taken up by afferent nerves and transported to the DRG cells. The levels of NGF also increase in the spinal cord after SCI. TrkA, which responds to NGF, is abundant in bladder afferents, especially C-fiber neurons. Hyperexcitability of bladder C-fiber afferent pathways causes or enhances neurogenic DO. BDNF is also increased in the bladder and the spinal cord after SCI. TrkB, which responds to BDNF, is expressed on larger-sized bladder afferent neurons, presumably Aδ-fiber, that express mechanosensitive receptors, ASIC and Piezo 2. Hyperexcitability of bladder Aδ-fiber afferent pathways causes or enhances DSD. Systemic application of BDNF antibodies reduces BDNF levels in the spinal cord and improves DSD. SCI: Spinal cord injury, DSD: Detrusor-sphincter dyssynergia, NGF: Nerve growth factor, DRG: Dorsal root ganglion, DO: Detrusor overactivity, BDNF: Brain derived neurotrophic factor, TrkB: Tropomyosin receptor kinase BThe immunoreactivity of TrkA, a high-affinity NGF receptor that is predominantly expressed in C-fiber afferent neurons, is increased in bladder afferent neurons of SCI rats.[84],[85] The NGF-TrkA axis is one of the important regulators of TRPV1 expression, spatial distribution, and activation thresholds in sensory neurons.[86],[87] A novel HSV vector-mediated neuronal labeling technique indicated that SCI induces expansion of the TRPV1-expressing C-fiber cell population, which might contribute to C-fiber afferent hyperexcitability.[88] TRPV1 upregulation is closely related to NGF overexpression after SCI. The systemic administration of TRPV1 or TRPA1 antagonists reduced both bladder contraction frequency and bladder hyperactivity.[89],[90] NGF neutralization downregulates NGF levels both at the bladder and the spinal cord and inhibits bladder hyperactivity along with reduced TRPV1 and TRPA1 expression in L6-S1 DRG.[77] Taken together, NGF is probably produced in the bladder after SCI, contributing to C-fiber afferent hyperexcitability mediated through TRP channels including TRPV1 and TRPA1, inducing the emergence of bladder overactivity.
Brain-derived neurotrophic factor
BDNF levels in the bladder and spinal cord are upregulated as early as 4–5 days after SCI in rats and mice.[84],[91],[92] BDNF induces various physiological and pathological changes by acting mainly on TrkB, a high-affinity, ligand-specific receptor of BDNF found in many neurons in the spinal cord and primary afferent pathways.[93] Although TrkB is expressed in both large (Aδ-fiber) and small (C-fiber) primary afferent neurons, higher TrkB expression is seen in large-sized, Aδ-fiber bladder afferent neurons [Figure 4].[85],[94]
In both SCI rats and mice, the afferent limb of micturition reflexes inducing bladder overactivity possibly consists of C-fiber afferents because capsaicin pretreatment significantly reduced bladder hyperactivity in both species.[51],[52] Previous studies reported that BDNF inhibition improved voiding function in chronic SCI rats whereas BDNF inhibition initiated during the post-SCI spinal shock phase resulted in the enhanced bladder overactivity, suggesting that BDNF in the early phase of SCI contributes to C-fiber-mediated bladder overactivity.[92],[95]
BDNF neutralization in 4-week-old SCI mice increases voided volume and voiding efficiency.[91],[92] In SCI mice, periodic reductions of EUS-EMG activity are observed during voiding bladder contractions, which coincides with notch-like reductions in intravesical pressure, reflected as urethral synergic relaxation that promotes voiding [Figure 3].[19] The durations of reduced EUS-EMG and notch periods are increased after BDNF neutralization, indicating improved urethral synergic relaxation during the voiding phase in SCI mice.[91],[92]
Acid-sensing ion channels (ASICs) expressed by sensory neurons might also be a molecular target of BDNF in bladder afferent pathways. Although ASICs were originally identified as receptors activated in response to diminished extracellular pH,[96],[97] they were later found to also have mechanosensory functions.[98] ASIC3 receptors are expressed in TRPV1-expressing, unmyelinated C-fiber neurons and in mechanosensitive myelinated A-fiber neurons in DRG.[99],[100] The ASIC2 channel, which is also a BDNF signaling target, regulates sensory mechanotransduction.[97] In the recent study, ASIC2 and ASIC3 transcripts in L6-S1 DRG were upregulated in SCI mice, which were suppressed after BDNF neutralization. By contrast, TRPV1 expression in L6-S1 DRG, which was increased after SCI, was not altered after BDNF neutralization.[91] Thus, BDNF might increase mechanotransduction through Aδ-fiber bladder afferent pathways to enhance the bladder-to-EUS reflex, leading to DSD and inefficient voiding after SCI [Figure 4].
Targeting p75 neurotrophin receptors
Mature BDNF and NGF are enzymatically processed within secretory vesicles from their proneurotrophins (proBDNF/proNGF) before release.[101] Under pathological conditions, their overexpression exceeds the processing rate leading to the unregulated release of proneurotrophins, which differ from mature forms in their affinity for the p75 neurotrophin receptor (p75NTR), whose expression is altered following SCI in the bladder and neuronal pathways governing micturition.[102],[103],[104] Furthermore, proBDNF/proNGF preferentially activates the p75NTR-sortilin complex. Sortilin is a transport protein involved in the organization of intracellular cargo between membrane compartments. When activated by proneurotrophins in conjunction with p75NTR, it can induce apoptosis in many cell types.[105] The mature neurotrophins activate their cognate Trk and p75NTR heterodimer, promoting survival and differentiation.
The modulator of p75NTR, LM11A-31, mimics the binding activity of the loop one domain of NGF and competitively antagonizes proneurotrophin binding to the p75NTR-sortillin dimer.[106] However, it can also potentially promote p75NTR-associated signaling through disinhibition and/or activation of the TrkA/BNTR-p75 complex.[107] LM11A-31 reportedly ameliorates DSD and DO in SCI mice and also blocks the SCI-related urothelial damage and bladder wall remodeling.[104],[108] Thus, drugs targeting p75NTR can modify DSD and/or DO in SCI and therefore assist in identifying underlying pathophysiological mechanisms and have therapeutic potential in SCI.
Potential Targets for Detrusor-Sphincter Dyssynergia/Inefficient Voiding after Spinal Cord InjuryAδ-fiber-targeting treatment
Ivermectin, which has been approved by the Food and Drug Administration for parasitic infections, activates a chloride flux in neurons expressing exogenous glutamate-gated chloride channel receptors (GluClRs), thereby shunting excitatory impulses causing hyperpolarization. Ivermectin-induced activation of mutant glycine receptors delivered to Aδ-fiber bladder afferents improves DSD and inefficient voiding in SCI mice, as shown before.[109] The α1 glycine receptor subunit with double mutation (G2M) has a larger single-channel conductance, increasing the sensitivity to ivermectin almost 100-fold higher than wild-type glycine receptor. G2M can be delivered specifically to Aδ-fiber bladder afferent neurons by NF 200 (NF200) promoter-driven HSV vectors targeting NF-expressing Aδ-fiber neurons [Figure 5]. Histological studies show cell hypertrophy of Aδ-fiber bladder afferent neurons labeled by NF200 promoter-driven HSV vectors in SCI mice.[109] Ivermectin-induced activation of G2M expressed in Aδ-fiber afferent neurons inoculation of NF200 promoter-driven HSV-G2M vectors into the bladder wall increases voiding efficiency and periods of reduced EUS-EMG activity during voiding bladder contractions.[109] This also reduces the expression of Aδ-fiber-related mechanosensitive channels (ASICs, Piezo) in L6-S1 DRG, without altering the C-fiber-related channel (TRPV1) expression.[109] Thus, the suppression of Aδ-fiber bladder afferent activity can potentially improve DSD and inefficient voiding in SCI [Figure 4].
Figure 5: Schema of replication-deficient herpes simplex virus (HSV) vectors. (a) The vector backbone vLG is generated from the HSV KOS strain in which BAC sequences are inserted into the TK locus (UL23). Deletions are introduced in the internal repeat region and the genes encoding immediate early proteins ICP4 and ICP27, rendering the vector replication-defective. The Gateway destination cassette is inserted into the remaining latency locus, replacing the latency promoter elements while maintaining a wildtype copy of ICP0 and the surrounding CTCF chromatin boundary elements. (b) To generate afferent neuronal subtype-targeted expression vectors, transgenes are recombined into the vector backbone via the Gateway cassette. Individual promoter sequences (1284 bp TRPV1 promoter [TRPV1p], 932 bp CGRP promoter [CGRPp], 553 bp CMV promoter [CMVp], and 970 bp NF200 promoter [NF200p]) incorporating a Kozak consensus translation initiation sequence are inserted into the pENTR1A transfer vector, which contains attL sites for site-directed recombination with the attR-containing vector backbone. These Gateway plasmids are then recombined into the vLG vector backbone to generate the experimental vectors. (c) Schema of vectors. Replication-deficient HSV vectors in combination with wild type (upper) and the double mutant (G2M) (lower) α1 glycine receptor subunit gene. The study (Saito, et al., 2019[107]) utilized a chemogenetic approach using a G2M receptor with increased sensitivity to ivermectin, in combination with replication-defective HSV vector-mediated gene delivery methods. HSV: Herpes simplex virusPiezo targeting treatment
Piezo1 and Piezo2, mechanosensitive ion channel proteins, are mainly expressed in the bladder and neurons, respectively. Piezo2 is mechanically activated and expressed in a subpopulation of sensory neurons, which is classified as low-threshold mechanosensory neurons (LTMR) that detect the direction of stimulus movements.[110],[111] A decrease in BDNF expression is associated with morphological polarization of Aδ-LTMR, leading to failure of direction-selective responses in these neurons.[112],[113] Piezo1 and Piezo2 channels are also expressed in the bladder epithelium and afferent pathways that can control low-threshold bladder-stretch sensing and micturition reflexes in mice.[114],[115]
Time-course changes after SCI reveal that TRPV1 and ASIC1-3 on L6-S1 DRG are increased early during the 2–4 weeks' period postinjury, but Piezo2 is increased in the later phase at 6 weeks' postinjury.[116] Intrathecal treatment of GxMTx4 (Piezo blocker) improves C-fiber-related bladder overactivity, the duration of EMG reduction time of the urethral sphincter, and voiding efficiency in SCI mice, as shown in our recent study.[116] Thus, treatments targeting Piezo2 channels in afferent pathways might improve both storage and voiding dysfunction after SCI.
Antifibrosis treatment
Urological diseases such as chronic bladder inflammation, benign prostate hyperplasia, and neurologic LUTD are often associated with bladder fibrosis.[117],[118],[119] Transcripts of type 3 collagen, hypoxia-inducing factor-1α, transforming growth factor (TGF)-β1, and fibroblast growth factor (FGF) are increased in the bladder of SCI rats.[120],[121] Inefficient voiding due to DSD induces bladder distention, which evokes bladder ischemia, followed by bladder fibrosis.[119] Bladder fibrosis with dense extracellular matrix deposition further deteriorates voiding dysfunction with reduced detrusor contractility, making the bladder stiffer, and less compliant.
Nintedanib, which inhibits the expression of fibrosis-related factor receptors including vascular endothelial growth factor (VEGF), FGF, and platelet-derived growth factor (PDGF), shows a lower risk of tumor promotion and is approved as a therapeutic agent for idiopathic pulmonary fibrosis patients.[122] Our recent study reported that subcutaneous nintedanib treatment improves both storage and voiding dysfunctions, evident as increased voided volume per micturition and voiding efficiency in SCI mice.[121] Nintedanib administration into SCI mice downregulates fibrosis-related molecules in the bladder including TGF-β1 and collagen type 1 and 3.[121] Increased mRNA levels of TRPV1, TRPA1, P2X2, and P2X3 in lumbosacral DRG (C-fiber related) in SCI mice are significantly decreased, and the collagen deposition (trichrome staining) in the bladder is decreased after nintedanib treatment.[121] Therefore, antifibrosis treatment using nintedanib, which inhibits VEGF, FGF, and PDGF receptors, can improve LUTD because of the bladder fibrosis in SCI. Furthermore, nintedanib-induced improvement of the bladder storage dysfunction might be mediated by modulation of bladder C-fiber afferent activity as seen by the downregulation of C-fiber afferent markers.
SummaryVarious changes in the spinal/peripheral nervous systems and the LUT, including the bladder and the EUS seemingly contribute to neurogenic LUTD such as DO and DSD after SCI above the sacral level. Research using animal disease models is important to detect different pathophysiological mechanisms of LUTD. SCI animal studies indicate that the emergence of reflex bladder activity and development of neurogenic DO after SCI is partly due to plasticity in bladder C-fiber afferent pathways, which are silent under normal conditions. Furthermore, recent animal studies implicate that Aδ-fiber afferent pathways might be involved in the pathophysiology to induce LUTD such as DSD following SCI. The detection of different factors contributing to this neural plasticity might help uncover potential targets for better/new treatments of LUTD after SCI [Figure 6]. Further translational research based on data from animal studies is warranted for the future development of novel therapeutic modalities for treating SCI-induced LUTD.
Figure 6: Summary of the potential targets for the treatments of LUTD after SCI. Several targets for the better/new treatments of LUTD due to SCI were reviewed in this article. Some targets are responsible for the storage dysfunction and others are for the voiding dysfunction such as DSD. These targets or medications need to be translated to the clinical setting. Some of them including ivermectin, nintedanib, mucimol or baclofen (GABA agonists) might be repositioned to new indications. LUTD: Lower urinary tract dysfunction, SCI: Spinal cord injury, DSD: Detrusor-sphincter dyssynergiaAcknowledgment
Authors would like to thank the National Institutes of Health (R01DK129194) (NY and SK) and the Department of Defense (W81XWH-17-1-0403) (NY).
Financial support and sponsorship
The research work has been supported by grants from the National Institutes of Health (R01DK129194) (NY and SK) and the Department of Defense (W81XWH-
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