The TGF-β1 pathway is early involved in neurogenic bladder fibrosis of juvenile rats (2024)

Pediatric neurogenic bladder (PNB) is the progressive bladder dysfunction caused by impaired urinary sensible or voiding nerves, mostly due to various spinal nerves abnormality, ultimately resulting in renal dysfunction.^1,2 The prevalence of PNB is from 0.45 to 2.6% in children.³ PNB often leads to serious bladder dysfunction in children, such as decreased bladder compliance, increased intravesical pressure, delayed emptying, and other serious bladder dysfunction, manifested as urinary incontinence, dysuria, repeated urinary tract infection, upper urinary tract damage, seriously life-threatening to patients, causing great pain to patients and their families, seriously affecting work and study, and increasing social burden.⁴

Current medical management for PNB, such as clean intermittent catheterization, antimuscarinic drugs like oxybutynin, intravesical injection of biotoxins, and bladder augmentation surgery, can effectively relieve patients’ symptoms, but has little effect to prevent or delay the PNB bladder’s deterioration on functions and morphologies.⁵ Neuroanastomosis treatment for PNB has attracted worldwide attention recently,⁶ but its therapeutic effect is controversial, and its clinical application is limited.⁷ Our previous studies found that the bladder function could not be fully recovered after lumbosacral nerve transection and neurogenic bladder nerve anastomosis and recanalization, and bladder fibrosis occurred in PNB bladder over time.⁸ It is speculated that bladder fibrosis is an important factor affecting the therapeutic effect.⁹ Therefore, successful treatment of PNB requires not only restoration of bladder innervation but also prevention and treatment of bladder fibrosis. However, the mechanism of PNB bladder fibrosis is still unclear, and there is no ideal treatment. Therefore, it is necessary to strengthen the basic and clinical research of PNB fibrosis.

To clarify when and how bladder fibrosis occurs during PNB progression, we used juvenile Sprague-Dawley (SD) rats to create PNB models by cutting the bilateral lumbar 6 (L6) and sacral 1 (S1) spinal nerves, which simulate PNB caused by lumbosacral spina bifida or lumbosacral spinal cord and/or spinal nerve dysplasia in children,^10,11 and then we investigated whole neurogenic bladder’s progression changes like morphology, structure, and function, as well as the expression of transforming growth factor (TGF)-β1 fibrosis pathway-related proteins in the PNB rat models, which might help to elucidate the whole molecular mechanism of PNB development and suggest better treatment strategy.

Animals

Sixty-four 8-week-old healthy female juvenile SD rats (150 ± 9.6 g) were provided by the experimental animal center of the local Medical University. The animals were housed in the animal facility at 22 ± 1 °C with 45–55% relative humidity on a 12-h artificial light–dark cycle. The local medical ethical committee approved all animal procedures (approval number 2018-KY-86).

Experimental design

PNB juvenile rat model

The PNB juvenile rat models were created as previously described by cutting the bilateral lumbar 6 (L6) and sacral 1 (S1) spinal nerves, which simulate PNB caused by lumbosacral spina bifida or lumbosacral spinal cord and/or spinal nerve dysplasia in children.^10,11 In brief, after inhalation anesthesia with 2% isoflurane (R51022,WEST GENE, Shanghai china), a dorsal median incision was created to expose the dorsal and ventral roots of L6–S1. The ventral and dorsal roots of bilateral L6 and S1 were transected, and the root stumps were ligated and buried into an adjacent muscle to prevent spontaneous nerve regeneration. In the sham group, nerve roots were only exposed by surgical instruments without transection or any other operation. Animals were housed separately postoperatively and kept on a 37 °C heating blanket overnight. Food and water were available ad libitum. Penicillin (2 × 10⁶ U/day) was administered for 3 days postoperatively.

Experimental groups

Rats were randomly divided into 8 groups (4 spinal nerve amputation and 4 sham groups) at 3-, 6-, 12-, and 24-week post-operation, and each group has 8 rats.

Cystometry

Cystostomy in juvenile rats

After the juvenile rats were anesthetized and underwent nerve amputation or sham operation, cystostomy was performed immediately as follows: a 1-cm incision (fist incision) was made on the midline extending cephalad above the pubic bone. A 6-0 silk suture was passed around the vertex of the bladder. A small incision was made within the suture limits, following which the PE50 catheter with a flared tip was passed into the bladder about 0.3 cm long, and the suture was tightened around the catheter (Fig.1a). The bladder was flushed back and forth through the catheter to assure no leakage.

A second incision of around 0.5 cm in size and approximately 3.0 cm above the first incision and a third incision of about 1.0 cm in size at the posterior neck were made to create a subcutaneous tunnel. Subsequently, a trocar was passed through the abdominal muscles from these three incisions, and the PE50 catheter was then passed through the trocar. After removal of the trocar, the catheter emerged through the tunnel at the back of the neck and was fixed to the subcutaneous fascia tissue with a 4-0 silk thread (Fig.1b). Less than 4.0 cm of the catheter was left outside the skin to prevent the rat from biting the distal end. The cystostomy catheter was checked and cleaned every day for cystometry, as needed.

Cystometry through cystostomy catheter

The cystostomy catheters in all groups were connected to a peristaltic pump (3M, Saint Paul, MN) (Fig.1c) and urodynamic equipment (Dantec Menuet Electrons, Skovlunde, Denmark) via a three-way connector for both infusion and pressure recording (Fig.1d). Cystometry was performed by infusing warm saline (37–38 °C) with filling rate 6 ml/h in shams and 15 ml/h in the PNB group, and basal intravesical pressure, bladder leak point pressure (BLPP), bladder compliance, maximum cystometric capacity, and maximum bladder contracting pressure were recorded. Three consecutive cystometries were performed in each rat, with an interval of at least 30 min to maintain consistent bladder activity.

Collagen fiber staining

Bladder samples were fixed with 10% paraformaldehyde buffer, dehydrated, and embedded in wax. The paraffin-embedded tissues were cut in 4-μm sections on a rotary microtome (Leica, RM2016). The paraffin sections were dewaxed and hydrated, followed by: (1) Masson staining, in which the microscopic examination showed the collagen fibers stained blue, while muscle fibers, fibrins, and red blood cells stained red; and (2) Sirius red staining, in which the collagen fibers were red, and the background was yellow under an optical microscope. However, under polarized light, collagen type III showed as a thin green fiber, and collagen type I as a thick orange or bright red fiber.

Immunohistochemical staining

Paraffin sections were dewaxed and rehydrated. Endogenous peroxidases were blocked using 0.5% H₂O₂ in methanol for 10 min at room temperature (RT, 20 °C), followed by antigen retrieval with 1 mM Tris/EDTA (pH 9.0) and blocking in phosphate-buffered saline (PBS) supplemented with 2% bovine serum albumin. Subsequently, samples were incubated overnight at 4 °C with the following primary antibodies: rabbit anti-TGF-β1 Rabbit pAb (GB11179, Servicebio, Wuhan, China), anti-Smad2 Rabbit pAb (GB11511, Servicebio), and anti-Smad6 Rabbit pAb (GB11654, Servicebio) diluted in PBS supplemented with 0.3% bovine serum albumin and 0.3% Triton X-100. After washing in PBS, the samples were incubated with horseradish peroxidase-conjugated secondary antibodies, and goat anti-rabbit immunoglobulin (GB23303, Servicebio) for 1 h at RT, followed by washing, antibody–antigen reaction with 0.05%3,3’-diaminobenzidine tetrachloride, and dissolving in distilled water containing 0.1% H₂O₂. Light microscopy was carried out using a Leica microscope. For each sample, at least ten randomly selected areas were evaluated.

Western blotting

Bladder tissues were dissected, ground, and lysed in the Mammalian Cell Protein Extraction Reagent (CWBiotech, Beijing, China). Total protein concentration was determined using the Pierce BCA Protein Assay Kit (Trans, Beijing, China). For each sample, 20 µg of protein was loaded and separated by sodium dodecyl sulfate–polyacrylamide gel electrophoresis. Subsequently, the proteins were electrophoretic transferred to a polyvinylidene fluoride membrane. The membranes were blocked with 5% nonfat milk in Tris-buffered saline (pH 7.4) containing 0.1% Tween-20 (TBST), incubated overnight at 4 °C with primary antibodies—rabbit anti-TGF beta receptor I (GB11271, Servicebio), anti-Smad2 (D43B4, Cell Signaling Technology, Danvers, MA), anti-Smad6 (PA5-87457, Invitrogen, ThermoFisher Scientific), anti-Collagen I (PA5-95137, ThermoFisher Scientific), and anti-Collagen III (PA5-34787, ThermoFisher Scientific)—in TBST with 5% nonfat milk. The secondary antibody (GB23303, Servicebio) was used to incubate the membrane for 2 h at RT. Labeling was performed using a western blot imaging with the Image Lab Software (ChemiDoc MP system, Bio-rad, Hercules, CA). Density and area of the bands were quantitated.

Statistical analysis

Calculations were performed using the GraphPad InStat3 for Macintosh software. Overall significance level between the amputated and sham groups or among the amputated groups was analyzed by one-way analysis of variance, using the Dunnett and Tukey–Kramer multiple comparison tests when appropriate. Statistical significance was set at P < 0.05. The data are shown as mean ± SEM.

Impaired cystometry in nerve-amputated rats

Cystometry showed no significant differences among the sham-operated groups at 3, 6, 12, and 24 weeks. Basal intravesical pressure was 3.51–5.42 cm H₂O with normal bladder compliance during filling. Further, bladder volume was 2.1 ± 0.04 mL, and maximum bladder contracting pressure was 40 ± 3.7 cm H₂O during voiding (Fig.1e).

However, there was no obvious contracting/voiding phase in any of the spinal nerve-amputated groups. The BLPP occurred and increased in a time-dependent manner 6 weeks following the operation. Further, basal intravesical pressure and bladder volume significantly increased over time after 6 weeks post-operation in the nerve-amputated groups compared to the sham-operated group (P < 0.05; Fig.1f–i).

Gross morphological changes of bladder tissue

The bladder size in the amputated groups initially increased at 3 and 6 weeks but decreased at 12 and 24 weeks when compared to the sham-operated groups. Further, the thickness of the bladder initially decreased at 3 and 6 weeks but gradually became thicker 6 weeks post-operation. Conversely, the bladder weight continuously increased over time in the nerve-amputated compared to the sham-operated groups (Fig.2).

Disrupted bladder structure and increased collagen III in nerve-amputated rats

Masson staining showed that the normal connective tissues in the bladder wall disappeared in the amputated rats and the layered structure of the bladder gradually disintegrated. Further, the thickness of the bladder wall initially became thinner, then gradually thicker. Additionally, the lamina propria decreased, the interstitial tissue became fibrillated, the smooth muscle tissues thickened and hypertrophied, and intramuscular collagen fibers gradually increased (Fig.3).

Sirius scarlet staining of 3-, 6-, 12-week-amputated rat bladders showed no significant difference in collagen III and the ratio of type III/I collagen fibers, compared to related-sham groups (pictures not shown). But 24-week-amputated rat bladders by Sirius scarlet staining showed a significant increase in collagen III, and the ratio of type III/I collagen fibers was higher than the sham group (3.99 ± 0.91 vs. 0.87 ± 0.41; P < 0.05; Fig.4).

Increased fibrosis-related protein expression in nerve-amputated rats

Immunohistochemical staining showed that expression of TGF-β1 and its classical pathway key protein Smad2 increased, while pathway inhibitory protein Smad 6 decreased, in the nerve-amputated groups when compared to the sham-operated groups (Fig.5).

Further, western blot analysis showed that TGF-beta receptor I expression in the rat bladder of the 6-, 12-, or 24-week amputated groups was significantly higher than the sham group and increased over time (P < 0.05, P < 0.01; Fig.6a, b). Smad2 expression in the 6-, 12-, or 24-week amputated groups was also significantly higher than the sham group and increased over time (P < 0.05, P < 0.01; Fig.6a, c). Conversely, Smad6 expression was significantly lower than that in the sham group, decreasing over time (P < 0.05 or P < 0.01; Fig.6a, d). Additionally, collagen I and collagen III expression levels in the 6-, 12-, or 24-week amputated groups were higher than the sham group and increased over time (P < 0.05, P < 0.01; Fig.6a, c). However, collagen III increased more sharply, thus the ratio of collagen III/I increased in a time-dependent manner.

SD rats are often used to create neurogenic bladder animal models, which have advantages of high hom*ozygosity within strains, strong regeneration, and anti-infection ability.^10,11 Twelve-week-old rats undergo sexual maturation and are usually defined as adult rats, and the cystometry parameters of bladder capacity, bladder basal pressure, and voiding pressure in the normal rats over 8-week-old changed very little with time. Thus we selected 8-week-old SD juvenile rats for the experiments to create the PNB animal model.

The main clinical features of PNB are detrusor paralysis and continuous high pressure of the bladder by cystometry.¹² Our PNB model by L6 + S1 amputation was also detrusor paralysis without obvious bladder contracting/voiding phase and continuous high pressure of the bladder by cystometry. In early stage of post-amputation (3-, 6-week post-amputation), the elevation of basal intravesical pressure was less significant than the middle- and late-stage of post-amputation (12-, 24-week post-amputation), which may be related to the compensatory bladder enlargement and bladder wall thinning as we observed (Figs.2 and 3). While in the middle- and late-stage of post-amputation (12, 24 weeks), the basic intravesical pressure and BLPP become continuous significant higher pressure by cystometry (Fig.1), which might result from thicker and harder bladder wall (Figs.2 and 3). So our findings are similar to the current reports,¹² and made the more detailing supplements to the literature on the PNB cystometry changes.

Usually the pathophysiological changes of PNB are increased smooth muscle cell proliferation and extracellular matrix, collagen deposition, and bladder wall hypertrophy,¹³ and it was reported that collagen I and III are the main collagens deposited during bladder fibrosis, with an increase in the type III/I ratio.¹⁴ Our study also found the smooth muscle cell proliferation, extracellular matrix deposition, and bladder wall hypertrophy in the PNB rats obviously from 12-week post-amputation time by histochemical staining; but we only found collagen III deposition greatly and type III/I ratio increase from 24-week post-amputation by Sirius scarlet staining. However, molecular protein detection by western blot informed that both collagen III and collagen I proteins’ expression levels increased from 12-week post-amputation, and the increase of collagen III protein was more and earlier from 6-week post-amputation, so the collagen III/I ratio increased progressively from 6-week post-amputation. In addition, protein expression levels of TGF-β1, Smad2, and TGF-beta receptor I also increased progressively from 6-week post-amputation in the PNB groups by western blot, while findings of protein increase by histochemical staining were from 12-week post-amputation.

Some studies reported TGF-beta/Smad signaling pathway was involved in chronic bladder outlet obstruction, causing bladder fibrosis.^15,16 The reason is that high intravesical pressure could be the extra harmful stimulus to bladder smooth muscle cells, in which the protein kinases could be further activated to regulate cell function changes and activate fibrosis progression.^15,16 In heart and liver researches, they reported the same findings that pressure overload induced myocardial fibrosis,¹⁷ and stress activated protein kinases and initiated liver cells’ fibrosis.¹⁸ Our studies also found the fibrosis progression consistent with the intravesical pressure, especially with basal intravesical pressure, higher basal intravesical pressure, and severer fibrosis. It might be the constant high intravesical pressure initiating the fibrotic process, because high intravesical pressure started at least from 3-week post-amputation by cystometry, probably even earlier (Fig.1), but the TGF-β1, Smad2, and TGF-beta receptor I and collagen III proteins increased progressively from 6-week post-amputation by western blot findings (Fig. 6). But these guesses needs further verification.

The effect of TGF-β1 on fibrosis is clear, and the fibrogenic effect of TGF-β1 is closely related to its receptors. Three receptors specifically bind to TGF beta 1, namely, TGF beta R I, TGF beta R II, and TGF beta R III, and the combinations of TGF beta 1 and TGF beta R I and II form a complex responsible for information transmission.^15,19 Smad2 protein has been reported to be the first activated downstream molecule transmitting TGF-β1 signals. TGF-β1 initiates its signaling pathway by mainly binding with TGF-beta receptor I on the cell membrane. This process phosphorylates and activates the intracellular Smad2 and Smad3 proteins to form a complex, then transfers to the nucleus to regulate collagen and fibrin genes, induce extracellular matrix production, and increase expression of type I and III collagen proteins, stimulating cell hypertrophy and fibrosis.¹⁹ Some researchers found decreased collagen deposition and increased bladder compliance in TGF-β1-deficient bladder outlet obstruction mice, also suggesting that TGF-β1 is involved in the process of cell fibrosis in the bladder.²⁰ In our study, we found that the expression of TGF-β1 and its downstream protein Smad2, together with collagen III and collagen I in bladder smooth muscle cells progressively increased over time after nerve amputation. In contrast, the pathway inhibitor protein Smad6 progressively decreased over time both by staining and western blot. Further, our findings on bladder morphology, structure, and function, e.g., thicker bladder wall, progressive collagen (primarily collagen III) deposition in the bladder tissues, and aggravated collagen III/I ratio, also pointed out the gross fibrotic appearance. These findings together implied that the TGF-β1/Smad signaling pathway gradually activate and progress over time in the PNB groups. Therefore, we suggest that effective treatment of neurogenic bladder in children should be started early before the occurrence of bladder fibrosis.

TGF-β1/Smad pathway inhibitors have been reported as fibrotic treatment in the liver, lung, heart, and kidney^15,21; however, they have yet to be tested for bladder fibrosis. As such, future studies exploring TGF-β1/Smad pathway inhibitors to prevent fibrosis in neurogenic bladder are indeed needed, such as inhibition of Smad phosphorylation or TGF-β1 signal transmission using TGF-β1 receptor or other pathway protein inhibitors. We may explore these studies in the near future.

This study has some limitations, such as the rat model by cutting the bilateral lumbar 6 (L6) and sacral 1 (S1) spinal nerves, simulated PNB caused by lumbosacral spina bifida or lumbosacral spinal cord and/or spinal nerve dysplasia in children (the most common types in clinical practice).^10,11 Thus the model might not apply to other PNB caused by brain diseases (e.g., brain hypoxia bladder) or peripheral nerves damages (e.g., diabetic bladder). Moreover, we selected 8-week-old SD juvenile rats for the experiments, so it gave less information about neurogenic bladder in infants or newborns.

In conclusion, our study found that the main clinical features of PNB were detrusor paralysis and continuous intravesical pressure at least from 3-week post-amputation by cystometry, probably even earlier; the smooth muscle cell proliferation, extracellular matrix deposition, bladder wall hypertrophy, and increased TGF-beta/Smad signal proteins in the PNB rats obviously from 12-week post-amputation time by pathophysiological staining, while TGF-beta/Smad signaling protein expression level changes were found from 6-week post-amputation time. Thus biological molecular findings are earlier than the pathophysiological findings by various staining. Therefore, early prevention of bladder fibrosis by targeting TGF-β1/Smad pathway-related proteins once knowing the PNB diagnosis might be an alternative treatment for PNB.

Author notes

1. These authors contributed equally: Yan Chen, Yuan Ma.

Authors and Affiliations

1. Pediatric Urodynamic Center and Department of Pediatric Surgery, The First Affiliated Hospital of Zhengzhou University, 450052, Zhengzhou, China

   Yan Chen,Yuan Ma,Yulin He,Dong Xing,Erpeng Liu,Xinghuan Yang&Jian Guo Wen

2. Institute of Clinical Medicine, The First Affiliated Hospital of Zhengzhou University, 450052, Zhengzhou, China

   Yan Chen,Yuan Ma,Yulin He,Dong Xing,Erpeng Liu,Xinghuan Yang&Jian Guo Wen

3. Department of Urology, The First Affiliated Hospital of Zhengzhou University, 450052, Zhengzhou, China

   Wen Zhu&Qingwei Wang

Contributions

Y.C. and Y.M. conceived and designed the experiments, performed the experiments, analyzed the data, wrote the paper, prepared figures, reviewed drafts of the paper, redid the experiments, and revised the paper. Y.H., D.X., and E.L. repeated the experiments, analyzed the data, and reviewed drafts of the paper. X.Y. and Y.H. performed the experiments and reviewed drafts of the paper. W.Z. and Q.W. contributed materials and reviewed drafts of the paper. J.G.W. conceived and designed the experiments, got the financial supports from the Foundations, provided the experimental platform and equipment, and reviewed drafts of the paper.

Corresponding author

Correspondence to Jian Guo Wen.

Competing interests

The authors declare no competing interests.

Patient consent

Patient consent was not required.

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