The animal experiments were approved by The First People’s Hospital of Yunnan Province, Affiliated Hospital of Kunming Science and Technology University (Kunming, China). Efforts were made to minimize the suffering of animals. All experimental procedures and protocols were in line with the recommendations of the Guide for the Care and Use of Laboratory Animals of the American National Institutes of Health.

A total of 100 Wistar male rats (weighing 190-200 g; aged 6 weeks) were purchased from the Laboratory Animal Center, Kunming Medical University (Kunming, China) for the following in vivo experiments. Streptozotocin (STZ) (Sigma-Aldrich; Merck KGaA, Darmstadt, Germany) injection was used for diabetic rat model establishment. STZ was dissolved in 0.1 mmol/l citric acid buffer (pH 4.5) to prepare 1% STZ solution. The rats were intraperitoneally injected with STZ solution (30 mg/kg). After 72 h, venous blood from the rat tails was collected, with blood glucose (BG) ≥16.7 mmol/l considered successful model establishment. The rate of successful modeling was 83% (83/100). Of the 100 rats, 10 died and seven rats were unsuccessfully modeled with BG <16.7 mmol/l. The rats successfully modeled were randomly grouped into a model group, DDAH2 group, DDAH2-NC group, short hairpin RNA (sh)DDAH2 group, shDDAH2-NC group, L-NNA group and L-NNA + DDAH2 group, with 10 animals in each group. Subsequently, 2.5×10¹⁰ PFU/ml DDAH2 lentivirus (2 µl), DDAH2-NC lentivirus, shDDAH2 lentivirus (2 µl), shDDAH2-NC lentivirus (2 µl) and shDDAH2-NC lentivirus (2 µl) were injected in the tail vein of the rats in the DDAH2 group, the DDAH2-NC group, the shDDAH2 group, the shDDAH2-NC group, and the L-NNA+DDAH2 group respectively. All lentivirus vectors were produced by Beijing Nuosai Biotechnology Co., Ltd. (Beijing, China). After 1 week, the injection was repeated again. Meanwhile, the NOS inhibitor L-NNA (5 mg/kg) was intraperitoneally injected into the rats of the L-NNA and L-NNA + DDAH2 groups following establishment of the rat models. The same dose of NOS inhibitor L-NNA was injected again after 20 h. The rats were housed at room temperature with a relative humidity of 50-60%, free access to food and water, and a 12-h light/dark cycle.

The H9C2 primary rat myocardial cell line (Institute of Biochemistry and Cell Biology, Shanghai Institutes for Biological Sciences, Chinese Academy of Sciences, Shanghai, China) was used for in vitro experiments. The cells were assigned into the model group (H9C2 cells treated with high glucose), DDAH2 group (H9C2 cells treated with high glucose and transfected with DDAH2 plasmid), DDAH2-NC group (H9C2 cells treated with high glucose and transfected with DDAH2-NC plasmid), shDDAH2 group (H9C2 cells treated with high glucose and transfected with shDDAH2 plasmid), shDDAH2-NC group (H9C2 cells treated with high glucose and transfected with shDDAH2-NC plasmid), L-NNA group (H9C2 cells treated with high glucose and incubated with 50 µmol/l L-NNA for 48 h) and L-NNA + DDAH2 group (H9C2 cells treated with high glucose, incubated with 50 µmol/l NOS inhibitor L-NNA for 48 h and transfected with DDAH2 plasmid). The cells were cultured in Dulbecco’s modified Eagle’s medium containing 10% fetal bovine serum (FBS) (all purchased from Sigma-Aldrich; Merck KGaA) 1×10⁵ U/l penicillin, and 100 mg/l streptomycin at 37°C with 5% CO₂. The medium was changed every 2 days. The cells were subcultured when cell confluence reached 80-90%. The cells prepared for high glucose treatment were cultured in culture medium with 30 ml/l glucose, and cells at the exponential growth phase were used for subsequent experiments.

According to the known DDAH2 sequence in NCBI (https://www.ncbi.nlm.nih.gov/nuccore/NM_212532.2), the DDAH2 plasmid, DDAH2-NC plasmid, shDDAH2 plasmid, and shDDAH2-NC plasmid were constructed by Sangon Biotech Co., Ltd., (Shanghai, China). At the same time, three different plasmids were screened to avoid off-target effects.

The third generation cells were detached by trypsin and inoculated into a 24-well plate for the cells to grow into monolayers with medium discarded. Transfection was performed using Lipofectamine 2000 (Invitrogen; Thermo Fisher Scientific, Inc., Waltham, MA, USA) according to the manufacturer’s protocol. The procedure was as follows: H9C2 cells were seeded into a 6-well plate at a density of 2×10⁵ cells/well and, when the cells had adhered to the wall, the medium was replaced with culture medium without penicillin/streptomycin 12 h prior to transfection. Subsequently, 100 µl liposome was diluted in 250 µl OPTI-MEM medium, triturated with a pipette and mixed prior to incubation at room temperature for 5 min. The plasmid vectors (4 µg) were diluted in 250 µl OPTI-MEM, triturated with a pipette and mixed prior to incubation at room temperature for 20 min, and then added to a 6-well plate containing 1.5 ml OPTI-MEM and mixed. The cells were incubated in a 5% CO₂ incubator at 37°C, and the medium was replaced with complete medium at 6 h. To screen out the stably transfected cells at 48 h post-transfection, the cells were seeded into G418 (1,000-2,000 µg/ml) medium for 4 weeks and the medium was replaced every 3-5 days.

Following lentivirus injection for 12 weeks, five rats in each group were heparinized by injection of 0.3% heparin (2 mg/kg) into the tail vein, intraperitoneally injected with 3% sodium pentobarbital (40 mg/kg) and anesthetized. Following fixation, the right common carotid artery of the rats was bluntly separated via a cervical median incision with the arteries ligated at the distal end of the heart. Subsequently, the proximal end of the heart was clamped and a small opening was cut in the artery wall to insert a catheter connected to the pressure transducer (Miller, Houston, TX, USA). The catheter was then placed into the left ventricle for several minutes with the ligature released. The catheter was connected to the Power Lab biometrics experiment system channel (AD Instruments, Oxford, UK) via a pressure transducer to measure the left ventricular end-diastolic pressure (LVEDP), left ventricular systolic pressure (LVSP), and the maximum rate of left ventricular pressure rise/fall (LV ± dp/dt).

The BG was measured in five rats selected from each group using the glucose oxidase method at 0, 5, 15 and 20 weeks. The steps of the glucose oxidase method were as follows: 10 µl plasma was added to 1.5 ml enzyme-buffer working solution, mixed and placed in a 37°C water bath for 10 min. A microplate reader (MK3, Thermo Fisher Scientific, Inc.) was used for assessment of the optical density (OD) values at 500 nm. The glucose levels were calculated according to formulas. The levels of total cholesterol (TC), triglyceride (TG) and fasting blood glucose (FBG) in the rats were analyzed using the Bayer 1650 blood chemistry analyzer (Bayer AG, Leverkusen, Germany). An enzyme-linked immunosorbent assay was used to detect the fasting insulin (FINS) levels of the rats in each group.

Following the analysis of blood biochemistry, the five rats in each group were sacrificed, limbs were fixed, the chest was opened in a sterile environment and the heart was removed. The heart was gently washed in phosphate-buffered saline (PBS) and then the residual blood in heart was extruded. The heart was trimmed and myocardial tissue samples of each group were obtained. The myocardial tissues were used for Masson staining and hematoxylin and eosin (H&E) staining, DDAH activity detection, reverse transcription-quantitative polymerase chain reaction (RT-qPCR) analysis and western blot analysis.

The myocardial tissues were fixed with 4% paraformaldehyde, embedded with paraffin, and cut into sections with a thickness of 4-µm. Following dewaxing, the tissue sections were stained with hematoxylin for 5 min, differentiated with hydrochloric acid ethanol, and then stained with Masson ponceau acid fuchsin solution for 5 min. Following rapid washing under water, the sample sections were stained with 1% phosphomolybdic acid for 3 min and stained with toluidine blue for 5 min prior to drying. Following this, the sections were mounted with gum and observed under a microscope (Nikon Ecliose 80i, Nikon Corporation, Tokyo, Japan).

The paraffin sections in each group were dewaxed and stained with hematoxylin for 5 min, followed by differentiation with ethanolic hydrochloric acid. The paraffin sections were washed and stained with eosin for 2 min. The sample sections were then quickly washed with water, dried, mounted with gum and observed under the microscope (Nikon Eclipse 80i, Nikon Corporation).

Following transfection for 24 h, the cells in each group were detached with trypsin and resuspended in serum-free medium containing bovine serum albumin (Sigma-Aldrich; Merck KGaA) for preparation of the cell suspension. Subsequently, 200 µl cell suspension was added to an 8-mm Transwell chamber (Costar, High Wycombe, UK) and placed in a 24-well plate. A total of 500 µl medium containing 20% FBS was added to the basolateral chamber for incubation for 24 h at 37°C with 5% CO₂. Cells in the apical chamber were wiped off with a cotton swab, washed with PBS 3-5 times, fixed with methanol for 20 min, and stained with 0.1% crystal violet for 20 min. Under an inverted microscope (Olympus, Corporation, Tokyo, Japan), five visual fields were randomly selected and images were captured. The experiment was repeated three times with the mean value obtained.

The ADMA concentration was determined by high performance liquid chromatography. Five rats were selected from each group, and 1 ml serum from the rat was added to 5-sulfosalicylic acid precipitation protein at 4°C and centrifuged at 2,000 × g for 5 min at 4°C. Following that, 10 µl serum or standard samples were added to 100 µl derivatization reagent (mixture of phthalaldehyde, borate buffer and D-mercaptoethanol), triturated with pipette fully, mixed and placed at room temperature for 3 min. The samples were then eluted using a linear gradient (mobile phase: 4% acetonitrile and 0.4% trifluoroacetic acid; flow rate: 0.2 ml/min). ADMA was then separated on columns in samples and internal standard samples, prior to being determined using a mass spectrometer (MS-2010; ADMAM/Z: 203, N2 flow rate: 4.0 l/min). Subsequently, the cells in each group were detached with 0.25% trypsin and centrifuged at 1,000 × g for 5 min at 4°C with the supernatant discarded. The cells were resuspended with 1 ml ice phosphate buffer (pH 6.5, 0.1 mol/l), split by sonication, and then centrifuged at 3,500 × g for 30 min at 4°C. Subsequently, the ADMA concentration in 50 µl of supernatant was measured as described above.

The activity of DDAH in myocardial tissues was determined as follows: 0.1 mmol/l L-proline (500 µl) were taken from a standard tube, and 50 µl myocardial homogenate and 50 µl cell lysate were taken from a testing tube and a control tube respectively. Subsequently, 100 µl ADMA standard solution (1 mmol/l) was added into the testing tube and an equal volume of PBS was added into the control tube and placed at room temperature for 2 h. To each tube, 10% trichloroacetic acid (0.5 ml) was added and centrifuged at 1,000 × g for 10 min at 4°C. Following the addition of 0.5 ml of supernatant into a clean glass test tube, 0.5 ml ddH₂O, 1 ml colorimetric solution containing 0.8% diacetyl monohydrazine and 0.5% antipyrine at the ratio of 2:1 were added, prior to sealing with preservative film. The tubes were placed in a water bath at 60°C for 100 min and cooled in ice water for several seconds without exposure to light, following which the OD value at 466 nm of each tube was determined with a full-wavelength UV spectrophotometer. The enzymatic activity of DDAH was the quantity of DDAH required to form 1 µmol/l L-proline per min at 37°C (expressed as U/g protein).

A NOS activity assay kit (Nanjing Jiancheng Biotechnology Co., Ltd., Nanjing, China) was used to measure NOS activity. The procedure was as follows: 50 µl supernatant or cell lysate of myocardial tissues following homogenization and centrifugation was added into a testing tube, and 50 µl ddH₂O was added into a control tube. In each tube, 200 µl substrate buffer, 10 µl accelerant and 100 µl color reagent were added, mixed and incubated for 15 min at 37°C. Following the addition of 100 µl clear reagent and 2 ml stop solution, the tissues were mixed and placed under plate reader (MK3, Thermo Fisher Scientific, Inc.) for assessment of the OD value at 530 nm. The NOS activity in each group was calculated according to following formulae: NOS activity = (OD _{testing tube}-OD _{control tube})/molar extinction coefficient × (the total volume of reaction liquid/the volume of sample) × (1/the time of reaction/the diameter of colorimetric ware)/the content of protein.

A NO content assay kit (Nanjing Jiancheng Biotechnology Co., Ltd., Nanjing, China) was used to determine the NO content. The procedures were as follows: 0.5 ml supernatant or cell lysate of myocardial tissues following homogeni-zation and centrifugation was added into a testing tube, 0.5 ml ddH₂O into the control tube and 0.4 ml ddH₂O and 0.1 ml 10 µmol/l standard liquid into the standard tube. Subsequently, 0.4 ml Reagent One and 0.4 ml Reagent Two were added into each tube and mixed fully with vortex and placed in a water bath at 37°C for 60 min. Subsequently, 0.2 ml Reagent Three and 0.1 ml Reagent Four were mixed fully for 30 sec, and allowed to stand for 40 min at room temperature. Following centrifugation at 3,500 × g for 10 min at 4°C, 0.8 ml supernatant and 0.6 ml color reagent were added, mixed thoroughly with a vortex and allowed to stand for 10 min. The OD values of the culture medium at 550 nm were measured using a microplate reader (MK3, Thermo Fisher Scientific, Inc.). The NO content in each group was calculated according to formulas: NO content (_µmol/gprot) = (OD _{testing tube}-OD _{control tube})/(OD _{standard tube}-OD _{control tube}) × concentration _{standard liquid (20 µmol/l)}/protein concentration _{testing sample (gprot/l)}.

Total RNA was extracted from the tissues and cells in each group using TRIzol Reagent (Takara Biotechnology, Co., Ltd., Dalian, China) with the RNA purity and concentration measured using a NanoDrop ND-1000 spectrophotometer (NanoDrop Technologies, Inc. Rockland, DE, USA). Subsequently, the PrimeScript RT reagent kit (Takara Biotechnology Co., Ltd.) was used for RT of the RNA into cDNA. The reaction system was as follows: 0.5 µl PrimeScript RT Enzyme mix, 4 µl 5X PrimeScript buffer, 1 µl RT primer, total RNA of 500 ng, with RNase Free ddH₂O added to a total PCR volume of 20 µl. The reaction conditions were as follows: At 37°C for 15 min and at 85°C for 5 sec. A UV spectrophotometer and 1% agarose gel were used to measure DNA concentration and purity (A260/A280 >1.8).

The prepared cDNA was subjected to the following experiments using the SYBR Premix Ex Taq II kit (Takara Bio, Inc., Tokyo, Japan) with glyceraldehyde-3-phosphate dehydrogenase (GAPDH) used as an internal reference. The reaction conditions were as follows: Pre-denaturation at 94°C for 10 min, 25 cycles of denaturation at 94°C for 1 min, annealing at 60°C for 45 sec and extension at 72°C for 2 min. The reaction system was as follows: 1 µl template cDNA, 0.4 µl forward primers and 0.4 µl reverse primers, 10 µl SYBR Premix Ex Taq, and 0.4 µl of ROX (50X), with ddH₂O added to a total PCR volume of 20 µl. The primers used are shown in Table I. All RT-qPCR experiments were performed using an ABI7500 quantitative PCR instrument (Applied Biosystems; Thermo Fisher Scientific, Inc.). The dissolution curves at 60-90°C were drawn to ensure that single products were amplified and the Cq value was used. The 2^−ΔΔCq method (21) was applied to detect the relative expression of each gene.

A total of 20 mg myocardial tissues from the rats in each group were supplemented with pre-cooled 2% sodium dodecyl sulfate at ratio of 1:20 (m:V), homogenized on ice for 10 sec in an electric homogenizer, and boiled at 100°C for 5 min. Following cooling, the tissues were centrifuged at 12,000 × g for 4 min at 4°, and the supernatant was collected as tissue protein samples. In each group, cells at the exponential growth phase were harvested following 72 h of culture, and total protein was extracted using the NucBusterä Protein Extraction kit (Novagen, Madison, WI, USA).

The concentration of protein samples was determined using a bicinchoninic acid kit (Pierce; Thermo Fisher Scientific, Inc.) with 30 µg protein sample in each protein lane adjusted by deionized water. Subsequently, the 10% SDS separation gel and spacer gel were prepared, and the samples were mixed with sample buffer prior to being boiled at 100°C for 5 min. After cooling to room temperature, each sample was subjected to electrophoresis by adding micro sampler into lanes. Subsequently, the protein on the gel was transferred onto a polyvinylidene fluoride membrane, which was then blocked with 5% skim milk overnight at 4°C. The membrane was incubated with the following diluted primary antibodies at 4°C overnight: Rabbit anti-rat protein arginine N-methyltransferase 1 (PRMT1; 1:1,000; cat. no. ab73246), rabbit anti-rat DDAH2 (1:500; cat. no. ab1383), rabbit anti-rat DDAH1 (1:500; cat. no ab2231), rabbit anti-rat collagen I (1:1,000; cat. no. ab34710), rabbit anti-rat matrix metalloproteinase 2 (MMP2; 1:2,000, cat no. ab37150) and rabbit anti-rat tissue inhibitor of metalloproteinase 2 (TIMP2; 1:500; cat. no. ab180630). This was followed by three PBS washes (5 min each time) at room temperature. All the above antibodies were purchased form Abcam (Cambridge, MA, USA). Subsequently, the membrane was incubated with secondary antibody, horseradish peroxidase-labeled goat anti-rabbit IgG (1:3,000; cat. no. ab6721, Abcam) at 37°C for 1 h, followed by three PBS washes (5 min each time). The membrane was then immersed in electroluminescence reaction liquid (Pierce; Thermo Fisher Scientific, Inc.) for 1 min at room temperature and the liquid aspirated, followed by covering with preservative film and observing under a chemiluminometer (Shanghai Tianneng Co., Ltd., Shanghai, China) with GAPDH (1: 2,500; cat. no. ab9485’ Abcam) as an internal reference. Finally, the ratio of the gray value of the target protein band/GAPDH protein band was considered the relative protein expression.

SPSS 21.0 (IBM Corp., Armonk, NY, USA) was used for statistical analysis. All experimental results were examined for Gaussian distribution and homogeneity of variance. Continuous variables are expressed as the mean ± standard deviation in the case of Gaussian distribution and as median (interquartile range) in the case of variables with non-normal distribution. Comparison of measurement data among multiple groups was performed using one-way analysis of variance, and post-hoc testing was conducted by Tukey’s test. In addition, repeated-measures analysis of variance was used to compare data at different time points. P<0.05 was considered to indicate a statistically significant difference.

The cardiac function was determined to examine the effect of DDAH2 on cardiac function in diabetic rats with myocardial fibrosis (Fig. 1A-D). Compared with the diabetic rats of the model group, a significant reduction in LVEDP was found in the diabetic rats of the DDAH2 group, whereas the levels of LVSP and LV ± dp/dt were increased (all P<0.05). By contrast, the level of LVEDP increased significantly and notable decreases in the levels of LVSP and LV ± dp/dt were observed in the diabetic rats of the shDDAH2 and L-NNA groups (all P<0.05). No notable differences in LVEDP, LVSP or LV ± dp/dt were observed in the diabetic rats of the model, DDAH2-NC, shDDAH2-NC and L-NNA + DDAH2 groups (P>0.05). Taken together, DDAH2 exhibited a protective effect on the cardiac function of diabetic rats with myocardial fibrosis.

The levels of biochemical indicators were detected for determination of the role of DDAH2 in diabetic rats with myocardial fibrosis (Fig. 2A-E). From week 5 following treatment, the levels of BG, TC, TG, FBG and FINS in the rats of the DDAH2 group were lower than those in the diabetic rats of the model group (P<0.05), whereas the levels of BG, TC, TG, FBG, and FINS were increased in the diabetic rats of the shDDAH2 and L-NNA groups (P<0.05). No significant differences in BG, TC, TG, FBG or FINS were found in the diabetic rats of the model, DDAH2-NC, shDDAH2-NC and L-NNA + DDAH2 groups (P>0.05). Taking these results into consideration, the positive role of DDAH2 was identified as it alleviated myocardial fibrosis in diabetic rats.

Masson staining and H&E staining were performed to further determine whether DDAH2 was involved in myocardial fibrosis in diabetic rats. Following Masson staining, collagen fibers turned blue and normal cells were stained red. In the diabetic rats of the model, DDAH2-NC, shDDAH2-NC, and L-NNA + DDAH2 groups, the myocardial cells were arranged loosely and disorderly with hypertrophied and deformed cardiac muscle cells. In addition, collagen fibers were distributed densely in the myocardial cells and blood vessels. Compared with the diabetic rats of model group, the myocardial tissues in the diabetic rats of the DDAH2 group were arranged regularly with reduced swelling and collagen fibers, whereas the arrangement of myocardial cells in the diabetic rats of the shDDAH2 and L-NNA groups was disordered with aggravated swelling and increased collagen fibers (Fig. 3A).

Following H&E staining, the myocardial cells in the diabetic rats of the model, DDAH2-NC, shDDAH2-NC, and L-NNA + DDAH2 groups were hypertrophied with obvious myocardial fiber damage and rupture. Less myocardial hypertrophy and necrosis, and generally complete cell morphology were observed in the DDAH2 group when compared with the model group. The diabetic rats in the shDDAH2 and L-NNA groups showed more hypertrophic and distorted myocardial cells, with disordered arrangement and an increase of intercellular space compared with the model group (Fig. 3B). These results showed DDAH2 attenuated myocardial fibrosis by reducing swelling and decreasing collagen fibers in diabetic rats.

Transwell, RT-qPCR and western blot assays were performed to evaluate the function of DDAH2 in the migration of H9C2 myocardial cells under high glucose conditions. The results of the Transwell assay (Fig. 4A) showed that the migration ability of the H9C2 cells in the DDAH2 group was significantly decreased compared with that in the model group (P<0.05), whereas the migration ability of H9C2 cells in the shDDAH2 and L-NNA groups was significantly enhanced (P<0.05). No significant differences in H9C2 cell migration were observed in the DDAH2-NC, shDDAH2-NC and L-NNA + DDAH2 groups (P>0.05).

In addition, the results of the RT-qPCR and western blot analyses (Fig. 4B and C) showed that, compared with the H9C2 cells of the model group, the mRNA and protein levels of collagen I, MMP2 and TIMP2 in the H9C2 cells of the DDAH2 group were significantly decreased (all P<0.05). The mRNA and protein levels of collagen I, MMP2 and TIMP2 in the H9C2 cells of the shDDAH2 and L-NNA groups were significantly increased, compared with those in the H9C2 cells of the model group (all P<0.05). No noticeable differences in the mRNA and protein levels of collagen I, MMP2, and TIMP2 were found in the model, DDAH2-NC, shDDAH2-NC, and L-NNA + DDAH2 groups (P>0.05). These result indicated that DDAH2 negatively affected myocardial cell migration.

In addition, the results (Fig. 4D and E) showed that, compared with the H9C2 cells in the model group, the H9C2 cells in the DDAH2 group showed significantly decreased mRNA and protein expression levels of PRMT1 but increased mRNA and protein expression levels of DDAH2 (all P<0.05). The H9C2 cells in the shDDAH2 and L-NNA groups exhibited increased mRNA and protein expression levels of PRMT1 but decreased mRNA and protein expression levels of DDAH2 compared with those in the model group (all P<0.05). No significant differences in the mRNA and protein expression levels of PRMT1 and DDAH2 were observed among the H9C2 cells in the model, DDAH2-NC, shDDAH2-NC and L-NNA+DDAH2 groups (P>0.05). No significant differences in the mRNA and protein expression levels of DDAH1 were found among the groups (P>0.05). Taken together, these results suggested that DDAH2 may induce the activation of DDAH in myocardial cells (H9C2) under high glucose conditions.

Finally, the regulatory association between DDAH2 and the DDAH/ADMA/NOS/NO pathway was investigated in diabetic rats with myocardial fibrosis. Compared with the rats in the model group, the rats in the DDAH2 group exhibited lower serum ADMA content but higher serum DDAH activity, NOS activity and NO content (all P<0.05); an opposite trend was observed in the shDDAH2 and L-NNA groups (all P<0.05). No notable differences in serum ADMA content, DDAH activity, NOS activity or NO content were observed among the model, DDAH2-NC, shDDAH2-NC, and L-NNA + DDAH2 groups (P>0.05) (Fig. 5A-D).

The results of the RT-qPCR and western blot analyses (Fig. 5E and F) showed that, compared with the diabetic rats in the model group, the mRNA and protein levels of PRMT1 were decreased whereas those of DDAH2 were increased in the myocardial tissues of diabetic rats in the DDAH2 group (all P<0.05). By contrast, the opposite trend was found in the shDDAH2 and L-NNA groups (all P<0.05). No significant changes in the mRNA and protein levels of PRMT1 or DDAH2 were shown among the model, DDAH2-NC, shDDAH2-NC and L-NNA + DDAH2 groups (P>0.05). No significant differences in the mRNA and protein levels of DDAH1 were observed among any groups (P>0.05). The above findings revealed that DDAH2 activated the DDAH/ADMA/NOS/NO pathway in diabetic rats with myocardial fibrosis.