Changes in pancreatic histology, insulin secretion and oxidative status in diabetic rats following treatment with Ficus deltoidea and vitexin
BMC Complementary and Alternative Medicine volume 17, Article number: 290 (2017)
The potential application of Ficus deltoidea and vitexin for the management of symptomatologies associated with diabetes mellitus (DM) has gained much attention. However, less firm evidence comes from data to augment our understanding of the role of F. deltoidea and vitexin in protecting pancreatic β-cells. The aim of this study was to assess histological and oxidative stress changes in the pancreas of streptozotocin (STZ)-induced diabetic rats following F. deltoidea extract and vitexin treatment.
F. deltoidea and vitexin was administrated orally to six-weeks STZ-induced diabetic rats over 8 weeks period. The glucose and insulin tolerances were assessed by intraperitoneal glucose (2 g/kg) tolerance test (IPGTT) and intraperitoneal insulin (0.65 U/kg) tolerance test (IPITT), respectively. Subsequently, insulin resistance was assessed by homeostasis assessment model of insulin resistance (HOMA-IR), quantitative insulin sensitivity check index (QUICKI) and the insulin/triglyceride-derived McAuley index. The histological changes in the pancreas were then observed by hematoxylin-eosin (H&E) staining. Further, the pattern of fatty acid composition and infrared (IR) spectra of the serum and pancreas were monitored by gas chromatography (GC) method and Fourier Transform Infrared (FT-IR) spectroscopy.
F. deltoidea and vitexin increased pancreatic antioxidant enzymes and promoted islet regeneration. However, a significant increase in insulin secretion was observed only in rats treated with F. deltoidea. More importantly, reduction of fasting blood glucose is consistent with reduced FT-IR peaks at 1200-1000 cm−1.
These results accentuate that F. deltoidea and vitexin could be a potential agent to attenuate pancreatic oxidative damage and advocate their therapeutic potential for treating DM.
Hyperglycaemia is the predominant cause of diabetic complications [1, 2]. Despite optimal treatment regimens, glucose fluctuation in the person with diabetes remains a major challenge . Acute glucose fluctuation in turn is responsible to influence the magnitude of oxidative stress. Importantly, oxidative stress has been postulated as a possible mechanism for diabetes-associated tissue and other systemic complications . It is thus justified to conclude that replenishment of insulin-producing pancreatic β-cells is crucial for treating diabetes and its complications , thereby overcoming the inadequacies of current treatment strategies.
It is now recognized that both major types of DM affects β-cells mass and insulin secretion . This fact has prompted renewed interest in targeting the pancreatic β-cell. The appreciation of the pancreatic β-cell offer promise in improving glycaemia control as well as potentially reducing the progression of diabetic complications. In most cases a single large dose of STZ has been carried out on laboratory animals for experiments attempting to determine strategies for replenishing β-cells [7, 8].
In Malaysia, F. deltoidea is frequently used for multiple purposes due to the high antioxidant activities. There is a large volume of published studies describing that the methanolic extracts of F. deltoidea plant leaves are rich sources of polyphenolics, flavonoids, and tannins [9, 10]. Vitexin was identified as a compound marker that associated with antioxidant and antidiabetic properties of F. deltoidea in animal models . F. deltoidea are known to be involved in lowering blood glucose level by enhancing the hepatic glycolytic enzymes in type 1 DM rats . There is also evidence that F. deltoidea [13, 14] and vitexin [11, 15] inhibits in-vivo and in-vitro α-glycosidase activity. In greater detail, Farsi et al.  revealed that F. deltoidea stimulates insulin secretion and blocks hepatic glucose production by regulating the expression of hepatic GK and PPARγ genes. Taken together, these findings imply that F. deltoidea and vitexin mimic the glucose-lowering effect of metformin as a popular synthetic drug for DM [17, 18]. Strikingly, new data showed the possibility of metformin to chemically protect β-cells survival . However, the information pertaining to the effects F. deltoidea and vitexin on the histological changes in the pancreas of rats are rather limited and inconclusive.
On the basis of these considerations, the present study was conducted to characterize histological and oxidative stress changes in the pancreatic of STZ-induced diabetic rats following F. deltoidea and vitexin treatment. In this study, it was also determined whether changes in tissue and blood serum would alter the composition of fatty acid and the pattern of FT-IR spectral.
Plant material and extract preparation
The leaves of F. deltoidea var. deltoidea were collected from Forest Research Institute Malaysia, Kepong, Malaysia in January 2015. The sample was then deposited at the Herbarium Unit, Universiti Kebangsaan Malaysia, Bangi and identified by Mr. Sani Miran with a voucher number Herbarium UKMB-40315. The leaves were washed thoroughly and over-dried at 37 ± 5 °C. The dried leaves were finely powdered using an electric grinder. For extraction, 100 g of powdered leaves was soaked in 1 L absolute methanol for three days at room temperature . Liquid extracts were concentrated using a rotary evaporator at 40 °C and subjected to freeze drying for 48 h. The extraction yield calculated was 10.6%.The extracts were kept in tightly closed glass containers and stored at −20 °C until further use.
The animal use and experimental protocols involved in the study were approved by the Universiti Putra Malaysia, Animal Care and Use Committee with an approval number: UPM/IACUC/AUP-R090/2014. A total of 30 male Sprague Dawley rats of four-week-old (mean body weight, 100 ± 5 g) were procured from Chenur Supplier Sdn. Bhd., Serdang, Selangor. The rats were housed at Laboratory Animal Facility and Management (LAFAM), Universiti Teknologi MARA, Puncak Alam, Selangor. The animals were acclimatized upon arrival for a week and were housed at a density of three per cage in a temperature controlled room (22 ± 1 °C and a 12 h light/dark cycle). The blood glucose levels and body weights of all animals were measured at the beginning of the study. The rats were identified with a cage card indicating project number, dose level, group, and animal number. They had access to standard rat chow (Gold Coin Holdings, Kuala Lumpur, Malaysia) and water ad libitum.
Diabetes-like hyperglycaemia was induced experimentally in rats through intraperitoneal injection of 0.5 ml STZ (Sigma-Aldrich, Deisenhofen, Germany) at a dosage of 60 mg/kg of body weight (b.w.) . After a week, animals with fasting blood glucose levels >11 mmol/L were considered diabetic .
Experimental design and procedure
The rats were divided into five groups of six rats per treatment group. The treatment group were normal control rats received saline (NC), diabetic control rats received saline (DC), Diabetic rats treated with 1000 mg/kg b.w. of metformin (DMET) , diabetic rats treated with 1000 mg/kg b.w. of F.deltoidea (DFD) , diabetic rats treated with 1 mg/kg b.w. of vitexin (DV) .
Metformin, methanolic extract of F. deltoidea and vitexin were dissolved in saline and treatments were given once daily via oral gavage for 8 weeks. Blood was sampled from the tail vein and fasting blood glucose was measured using a portable glucometer (Accu-Chek, Roche, Germany) at 1-week intervals.
At the end of the experiment, all animals were fasted overnight. Animals were then anesthetized with ketamine (80 mg/kg) and xylazine (8 mg/kg), followed by terminal exsanguination. Blood samples (10-15 ml) were collected via cardiac puncture from the rats into plain red-top tube containing no anticoagulants (BD Vacutainer®, USA). The blood samples were then centrifuged at 4000 g for 15 minutes, and serum was stored in aliquots at −80 °C. Triglycerides in serum were determined using an automatic analyser (Hitachi 911, Boehringer-Mannheim, Germany). Meanwhile, pancreas was carefully excised, rinsed in ice-cold saline and stored in 10% formalin for tissue characterization.
Glucose and insulin tolerence measurements
The intraperitoneal glucose tolerance test (IPGTT) and intraperitoneal insulin tolerance test (IPITT) were performed at the end of 8 weeks treatment on all experimental groups. These tests were performed with minor modifications following the method described by Abdollahi . The rats were fasted for 8 h prior to testing. For the IPGTT, glucose (2 g/kg) was injected intraperitoneally at time 0. Following day, the rats were intraperitoneally injected with insulin (1.5 IU/kg) for the IPITT. Blood glucose measurements from the tails were performed at 0, 30, 60 and 120 min. The blood glucose concentration versus time (minutes) was plotted and the area under curve (AUC) was calculated following the trapezoidal rule.
Fasting serum insulin
The levels of serum insulin were determined by Enzyme Linked Immunosorbent Assay kit specific for rat insulin (Cloud-Clone Corp., Houston, USA) as described by Zhang et al. . Serum was allowed to thaw and 50 μl serum was pipetted into duplicate wells followed by 50 μl of enzyme conjugate solution. This mixture was incubated for 1 h on a plate shaker (800 rpm) at 37 °C. The plate was inverted on an absorbent paper after the final wash. Afterward, 90 μl of substrate solution was pipetted and incubated at 37 °C. Finally, the reaction was stopped 15 min later by adding 50 μl of stop solution to each well. The optical density was read at 450 nm with microplate reader (Epoch Microplate Spectrophotometer, BioTek, USA). The values for the calibrators were used to plot a calibrator curve from which the values for the samples were extrapolated.
Determination of insulin sensitivity
Three indirect indexes for the assessment of insulin sensitivity were calculated using serum insulin, glucose and triglyceride at the end of the experimental period. The HOMA index uses the formula described by Matthews et al.  while the quantitative insulin sensitivity check index (QUICKI) is based on the logarithmic transformation. Accordingly, McAuley’s index  was calculated based on the increase of triglycerides levels and insulin according to the following equations:
The paraffin-embedded pancreas was sectioned at 4 μm using a semiautomated microtome (RM2155; Leica Micro-systems). The tissue sections were then mounted on glass slides using a hot plate (HI1220; Leica Microsystems). Afterward, the tissue sections were deparafinized by xylene and rehydrated by different graded ethanol dilution (100%, 90%, and 70%). The sections were stained with hematoxylin and eosin (H&E). All slides were examined using light microscopy (Motic BA410, Wetzlar, Germany) equipped with a digital camera (Moticam Pro 285A, Wetzlar, Germany) under a magnification of X200.
The amylin level in the serum was determined by using Rat Amylin Enzyme Immunoassay Kit (RayBiotech Incorporation, USA). Standards and reagents were prepared carefully according to the procedure in the instruction manual prior the assay. One hundred microliters of anti-amylin antibody was added to each well and incubated overnight at 4 °C. The solution was then discarded and washed four times by using 1X wash buffer. A 100 μl of each standard, sample and blank (assay diluent) were added in triplicates to the wells. The wells were then covered and incubated for overnight at 4 °C. The solutions were discarded and washed four times. An amount of 100 μl HRP-streptavidin solution was added to each well and incubated for 45 min at room temperature with gentle shaking. One hundred microliters of TMB one-step substrate reagent was added to each well and allowed to incubate for 30 min at room temperature in the dark with gentle shaking. Finally, 50 μl of stop solution was added to each well and the absorbance was immediately read at 450 nm wavelength using microplate reader (Epoch 2 microplate spectrophotometer, BioTek Instruments, Inc., Vermont, USA).
Preparation of tissue homogenates
The pancreatic tissue was homogenized in 10% (w/v) homogenizing buffer (50 mM Tris-HCl, 1.15% KCl pH 7.4) using a Teflon pestle (Glass-Col, USA) at 900 rpm. The homogenates were centrifuged at 9000 g in a refrigerated centrifuge (4 °C) for 10 min to remove nuclei and debris. The supernatant obtained was used for biochemical assays and FT-IR analysis. Protein concentration was estimated by the method of Lowry , using bovine serum albumin as the standard.
Estimation of MDA levels
The levels of MDA equivalents were determined in pancreas by TBARS assay kit (Cayman, MI, USA) as describe by Hardwick et al. . The absorbance was determined spectrophotometrically at wavelength of 540 nm using a spectrophotometer.
Assessment of antioxidant enzymatic activities
Glutathione peroxidase (GPx) activity was measured using assay kit (Cayman, MI, USA). The experimental procedures were carried out according to the manufacturer’s instructions . The measurement of GPx activity is based on the principle of a coupled reaction with glutathione reductase (GR). The oxidized glutathione (GSSG) formed after reduction of hydroperoxide by GPx is recycled to its reduced state by GR in the presence of NADPH. The oxidation of NADPH is accompanied by a decrease in absorbance at 340 nm. One unit of GPx was defined as the amount of enzyme that catalyzes the oxidation of 1 nmol of NADPH per minute at 25 °C.
Superoxide dismutase (SOD) activity was determined using assay kit (Cayman, MI, USA). This kit utilizes a tetrazolium salt for the detection of superoxide radicals generated by xanthine oxidase and hypoxanthine. One unit of SOD was defined as the amount of enzyme needed to produce 50% dismutation of superoxide radical.
Fatty acid analysis
Lipids from the serum and pancreas were extracted according to the methods described by Hajjar et al. . According to this method, 1 ml of serum were thawed at room temperature for 30 min and extracted using the Folch method  (chloroform:methanol, 2:1, v/v) containing butylated hydroxytoluene as antioxidant. Then, fatty acids methyl esters (FAME) were prepared using 0.66 N potassium hydroxide (KOH) in methanol and 14% methanolic boron trifluoride (BF3) (Sigma Chemical Co. St. Louis, Missouri, USA). The FAME were separated with an Agilent 7890A Series GC system (Agilent Technologies, Palo Alto, CA, USA) using a 30 m × 0.25 mm ID (0.20 μm film thickness) Supelco SP-2330 capillary column (Supelco, Inc., Bellefonte, PA, USA). The fatty acid proportions are expressed as percentage of total identified fatty acids. One microlitre of FAME was injected by an auto sampler into the chromatograph, equipped with a split/splitless injector and a flame ionization detector (FID) detector. The injector temperature was programmed at 250 °C and the detector temperature was 300 °C. The column temperature program initiated runs at 100 °C, for 2 min, warmed to 170 °C at 10 °C/min, held for 2 min, warmed to 200 °C at 7.5 °C/min, and then held for 20 min to facilitate optimal separation. Identification of fatty acids was carried out by comparing relative FAME peak retention times of samples to standards obtained from Sigma (St. Louis, MO, USA).
Infrared spectroscopic experiments were performed using a Bruker 66 V FT-IR spectrometer (Bruker Corp., MA, USA) that was equipped with a focal plane array detector. Twenty microliter of each homogenate sample was then deposited on a liquid cell (demounted cell) using a pipette according to the method reported by Demir et al. . All individual FT-IR spectra were recorded over the range 4000-400 cm−1 at room temperature. In order to resolve the overlapped absorption components in FT-IR spectra, second derivative spectra were calculated using Savitzky–Golay algorithm. All spectra processing was performed by using OPUS 7.0 software (Bruker Optics, GmbH). The peaks of each spectrum curve were then fitted and calculated. The region enriched vibration changes were compared to existing literature database towards providing chemical information on the targeted tissues. Absorptions belonging to fatty acyl chains, proteins and carbohydrates of biological samples are basically available in the 3020-2800 cm−1, 1700-1500 cm−1 and 1200-900 cm−1 spectral intervals, respectively .
The fasting blood glucose, IPGTT and IPITT data sets were analysed using repeated measures ANOVA. Meanwhile, one-way ANOVA analyses were done on insulin levels, insulin sensitivity indexes, oxidative stress marker, antixioxidant enzymes serum and pancreas fatty acids compositions data sets to investigate the differences among the treated groups. In both cases Duncan’s multiple comparison test was employed to elucidate significant means. Results were presented as the mean ± 1 SD. All analysis was performed at 95% confidence level.
Fasting blood glucose
The means and standard deviations of FBG in entire groups are given in Table 1. The FBG concentrations in the DC animals were increased by 50.65% compared to initial values, confirming the validity of the diabetogenic dose of STZ in this study. It is noticeable that the treatment for 8 weeks with either metformin or F. deltoidea or vitexin resulted in a significant reduction in FBG. The FBG decreased by 38.03% and 47.85% following F. deltoidea and vitexin treatment, respectively as compared to pre-treatment values. All treated diabetic groups depict significant changes at week 6 of treatment.
Glucose and insulin tolerance
The blood glucose concentrations were measured for the period of 0-120 min after glucose and insulin infusion. The DC rats displayed impairments in glucose (Fig. 1a) and insulin responses (Fig. 1b), as characterized by increased area under the curve (AUC). Conversely, both F. deltoidea and vitexin treatments marginally improved whole-body blood glucose disposal in diabetic rats as indicated by lower AUCs compared to the NC group.
As depicted in Table 2, serum insulin levels, HOMA-B, QUICKI and McAuley index was alleviated markedly in the DC rats compared to the NC rats. It was also found that STZ associated with a significant increase in serum triglyceride and HOMA-IR index. Notably, F. deltoidea increased the secretion of insulin. Adhering to three indirect indexes used to predict insulin sensitivity, both F. deltoidea and vitexin had a significant impact in lowering insulin resistance. Triglyceride levels also decreased in both the DFD and DV rats. Nevertheless, both treatments failed to improve the HOMA-B scores.
The histopathology of rat pancreas was shown in Fig. 2. Microscopic investigation of pancreas sections of NC rats showed the normal appearance of islets of Langerhans. The islets appeared lightly stained than the surrounding acinar cells. The acinar cells are formed of pyramidal cells with basal nuclei and apical acidophilic cytoplasm (Fig. 2a). However, the DC rats showed pathological changes of both exocrine and endocrine components. The acinar cells were swollen and small vacuoles were observed in almost all acinar cells. Interlobular ducts were lined with flattened epithelium. Islet β-cells are almost entirely lost in STZ-treated rats (Fig. 2b). Similar findings were obtained in the DMET rats. In fact, both the DC and DMET pancreas associated with different intensity of eosin as compared to the NC rats (Fig. 2c). On the other hand, DFD and DV groups depicted evidence of cellular regeneration among the islets of Langerhans (Fig. 2d and e). Atrophic change of the acinar cells was less severe and the border between exocrine and endocrine portions became more distinct.
Oxidative stress marker and antioxidant enzymes
Table 3 summarizes the results for the effect of F. deltoidea and vitexin on pancreas lipid peroxidation and the activities of antioxidant enzymes. There was a significant decrease in the activity of SOD and GPx upon injection of STZ, reflecting the depletion of endogenous antioxidant enzymes activities in serum. Strikingly, administration of F. deltoidea to diabetic rats resulted in a significant increase in the SOD and GPx values relative to the DC group. Although GPx markedly increased following vitexin treatment, the SOD activity remained low throughout the studied period. Nevertheless, the DFD and DV groups associated with a significant reduction in pancreatic TBARS.
As shown in Fig. 3, serum amylin levels were significantly increased in the DC group. However, metformin and F. deltoidea treatments significantly reduced the levels of serum amylin.
Serum fatty acid profiles
Table 4 lists the percentages of total fatty acids in the serum. It was demonstrated that the total serum saturated fatty acid (SFA), monounsaturated fatty acid (MUFA), and polyunsaturated fatty acids (PUFA) were roughly similar across the treatment groups. However, there were significant differences (P < 0.05) in the serum fatty acid profiles of DV group. The DV animals had more total n-3 PUFA in their serum as compared to the DC and NC animals. The serum docosahexaenoic acid (DHA) was clearly the highest in the DV groups.
Fatty acid profiles of the pancreas
It is noticeable that the injection of STZ had insignificant effect on the total SFA and PUFA (Table 5). However, the DC group clearly had the lowest level of total MUFA. Similarly, the DV animals experienced significant decline of total pancreas MUFA at the end of the trial. Oleic acid was significantly decreased in both groups. However, the total n-3 PUFA levels in the pancreas of DV animals was more than three-fold and two-fold higher than those found in the NC and DC animals, respectively.
FT-IR spectra of the serum
The FT-IR spectra changes in response to alterations in tissue and serum glucose upon F. deltoidea and vitexin treatment were investigated. In general, all animal groups had strong bands at 1660 cm−1, arising from C = O stretching vibration of the peptide group and another broad peak at 3100-3600 cm−1 corresponding to stretching of the hydroxyl groups (Fig. 4a). As shown in Fig. 4b, the most obvious differences between experimental groups were found in the range of 1200 and 1000 cm−1. This peak indicates the presence of sugar.
The second derivative spectra below shows that the glucose peak intensities at 1080 and 1036 cm−1 increased in the DC rats with high blood glucose. The intensity of glucose peak was nevertheless decreased among all treated groups (Fig. 5b-d), which is consistent with the reduction of FBG concentrations (Table 1). This data indicates a possible correlation between the peak intensities at 1080 and 1036 cm−1 and the blood glucose concentration obtained by conventional methods. Unexpectedly, the IR spectra of serum from the DMET and DV rats elicited a greater increase in the intensity of fructose peak at 1057 cm−1. However, lesser intensity of fructose band was observed in the IR spectra of DFD group.
FT-IR spectra of the pancreas
The FT-IR spectra of pancreas tissues from different groups are shown in Fig. 6a. For detailed analysis of IR spectra, the region was divided into two distinct frequency ranges, namely 3000-2800 cm−1 (Fig. 6b) and 1500-1050 cm−1 (Fig. 6c). It was noticed that the IR spectra of pancreas are different at three regions which were 3000-2800 cm−1, 1450-1380 cm−1, and 1200-1000 cm−1. These observations imply that the structural and functional changes in pancreas are somehow related to lipid, protein and glucose specific absorption band.
The second derivative analysis showed that the most dominant peak in the region of 3000-2800 cm−1 had decreased to levels far below normal in the DC and DMET groups. Interestingly, the spectra of pancreas from the DFD and DV rats are almost similar to that of the normal spectrum (Fig. 7c and d). These results suggest that lipid is involved in pancreatic regeneration.
It was found that the DC animals are associated with a lower intensity of band within 1440-1390 cm−1 region (Fig. 8a), indicating the diminished of methyl groups for enhancing pancreatic β cell regeneration. Similar FT-IR spectra were obtained from the DMET groups as illustrated in Fig. 8b. However, second derivative spectra showed the reappearance of weak peak at 1422 and 1408 cm−1 in the DMET group. As seen in Fig. 8c, the spectra of DFD group displayed a clearer reappearance of the methyl band with minor shifts. Meanwhile, similar spectral characteristics seen in the NC animals illustrated in the spectra of DV group (Fig. 8d).
Figure 9a demonstrates that the pancreatic tissues from NC animals depict the presence of five significant peaks in the region of 1190-1100 cm−1. However, the intensity and frequency of the sugar band of the DC group was reduced and shifted especially between 1130 and 1106 cm−1. Strikingly, the spectra of DFD and DV treated groups do contain some similarities to the NC group. Both groups displayed five peaks within the region, suggesting that glucose is important elements toward the regeneration of pancreatic β-cells.
Profiles of IPGTT and IPITT showed that STZ induction resulted in impaired glucose and insulin tolerance. STZ induced insulin resistance on rat was then confirmed by HOMA-IR, QUICKI scores and McAuley indexes [34, 35]. In line with previous observations, the activity of pancreatic antioxidant enzymes decreased in parallel with islet cell degeneration seen in sections stained with H&E . The main finding of this study was that F. deltoidea and vitexin are associated with regenerative effect on the islet cells. In support, the levels of FBG and serum triglyceride decreased significantly following these treatments. These findings also highlighted the changes in serum and pancreas was somehow related to fatty acid composition and FT-IR spectra.
Histological examination of the pancreas of DC rats showed a complete destruction of pancreatic islet (Fig. 2b). The acinar cells were swollen and small vacuoles were observed in almost all acinar cells. The substantial drop in HOMA-B supports the deterioration of β cell function in animal models as lower HOMA-B index reflect the failure of pancreatic β-cell function . This is in agreement with studies demonstrating that a single dose of 60 mg/kg STZ is capable to induce pancreatic β-cell destruction in rats and subsequent reduction of insulin secretion [38, 39]. One particular interesting finding was that DFD and DV rats had increased the size and density of dispersed islet tissue (Fig. 2d and e). It currently accepted that targeting the pancreatic β-cell is the most promising strategies for treating diabetes . Several plant extracts have been previously reported to be associated with the regeneration of pancreatic β-cells in STZ-treated diabetic rats [41,42,43]. More important, serum insulin levels markedly increased in the DFD rats.
Both GPx and SOD activities decreased in the pancreas of DC rats, suggesting that pancreatic oxidative stress was stimulated. Similar results have also been reported in the different animal models [44, 45]. The activities of pancreatic antioxidative enzymes (GPx and SOD) are known to be diminished in the islet cells of diabetic animals as β cells are considered to be low in antioxidant defense and susceptible to oxidative stress [46, 47]. Earlier work by Tiedge et al.  showed that islets contain only 2% GPX1, and 29% SOD1 activities as compared to liver. It is therefore possible that, pancreatic SOD is highly responsive to hyperglycaemia than GPx. In agreement with the findings, Zhou et al.  reported a significant decrease in SOD mRNA expression in pancreatic β cells of diabetic animals. These results supported the hypothesis that the acceleration of cell death could be attributed to reduced pancreatic antioxidative enzymes. Importantly, increased pancreatic antioxidant capacity was remarkable in the pancreas of DFD and DV rats.
It is interesting to note that serum amylin was slightly increased in STZ treated rats, thereby may explain partly the degeneration of the islets of Langerhans. This argument is established based on the fact that amylin is implicated in the loss of β-cells [50,51,52]. It has been reported that amylin induces apoptosis in pancreatic β cell by increasing the expression of c-Jun, a gene that is involved in the apoptotic pathway . Cai et al.  later showed the elevation of amylin in acute inflammation-related pancreatic disorders. Furthermore, the results of the in vitro study demonstrated that treatment of INS-1 cells with amylin enhances cell death, inhibits cytoproliferation, and increases autophagosome formation . The major findings of the current study illustrated that F. deltoidea inhibited the amyloid aggregation but vitexin does not. Indeed, the ability of plant extracts to inhibit the formation of amylin has been reported in several studies [56, 57]. In parallel with histological changes of the pancreas, these findings raising the possibility that amylin could be part of the trigger for β-cell regeneration .
Disturbances of the fatty acid composition may be critical to explain the pancreatic β-cell destruction . We are proceeding to describe that endogenous production of stearic acid was increased while total MUFA (oleic acid and palmitoleic acid) was decreased in the pancreas of diabetic rats. These findings align with other studies showing that stearic acid induced endoplasmic reticulum stress of pancreatic β-cells . In fact, a substantial increase in stearic acid content of pancreatic islets incubated in the presence of glucose had been previously reported .
The dramatic decrease in pancreas oleic acid and palmitoleic acid was also observed following STZ-induced diabetes, suggesting the progression of pancreatic β-cell death. Cnop et al.  demonstrated that oleic acid exert protective effects against apoptosis in the pancreas. Notably, oleic acid was more potent than palmitoleic acid against palmitic acid-induced apoptosis in pancreatic AR42J cells . High concentrations of oleic acid have been pointed out to be effective in reversing the inhibitory effect in insulin production [64,65,66]. Nevertheless, Kudo et al.  provide evidence that chronic exposure to oleic acid led to the continuous excitation of β-cells, depletion of insulin storage, and impairment of glucose-stimulated insulin secretion (GSIS). This discrepancy can be justified by the fact that oleic acid increased the expression of GLUT2, which may partially contribute to the increased basal insulin secretion  but enhanced the levels of intracellular free Ca2+, which most likely accounts for the decrease of GSIS .
In the current study, it was shown that vitexin prevents β-cell destruction. This finding is likely due to the enrichment of endogenous n-3 fatty acid. The beneficial effects of n-3 PUFA at the pancreatic level has been previously explained by Bellenger et al. . More details, Hwang et al.  pointed out that n-3 PUFA enrichment might partly prevent the STZ-related pancreatic islet damage by upregulating the basal activity of autophagy and improving autophagic flux disturbance. However, vitexin had no significant effect on insulin secretion.
Another important finding of the present work is that the changes in serum and tissue are supported by FT-IR peaks. These findings were consistent with previous results showing that alterations in the IR spectral signature are related to subsequent changes in tissue structure and function . In particular, reduction of FBG is reflected by reduced FT-IR peaks at 1200-1000 cm−1. It is also observed that STZ decreased the intensity of glucose peak in the pancreas of diabetic animals, suggesting glucose deprivation within the cell. There is increasing acceptance of the idea that inadequate tissue glucose causes overproduction of ROS . Indeed, slight increases in pancreatic TBARS level was also found in DC rats. Most in-vivo and in-vitro studies have demonstrated that glucose is the key for β cell replication [74,75,76]. However, Assmann et al.  showed that the effects of glucose on β-cell growth and survival are insulin dependent process.
It is also noticeable that the intensity of lipid methylene in the pancreas is markedly attenuated by diabetes. The similar effect of diabetes has been reported by Réus et al. . Firmed convincing results have been published on the alterations of pancreatic structure and derangements in the lipid metabolism evoked by STZ . The absence of any recognizable islets of Langerhans in response to STZ strengthens the link between pancreatic structure and methylene peak. In fact, Nolan et al.  showed that diabetes apparently causes lipid damage in the pancreas as it is essential for insulin secretion as well as to compensate for insulin resistance. Consistent with the earlier finding, we suggest that disappearance of methylene peak in IR spectra of diabetic pancreatic samples gave an important clue of destruction of the pancreas leading to impaired insulin secretion. The absence of methylene peaks along with glucose band in the IR spectrum of DC may further accentuate the initial interaction between role of insulin and glucose on β-cell regeneration and function. Strikingly, methylene, methyl and glucose peaks from the pancreas of both groups appeared almost similar to that of the normal spectrum, suggesting the suitability of FT-IR as a rapid and non-invasive detection method .
Despite the promising effects in reducing FBG and replenishment of β-cells in diabetic animals, FT-IR analysis revealed the presence of fructose peak with higher intensity in the serum of DMET and DV groups. It is important to note that fructose does not acutely raise blood glucose , thus, explains the reduction of FBG seen in the DM and DV groups. However, Jaiswal et al.  demonstrate that exposure to fructose induces cell-autonomous oxidative response through ROS production and thus impairs insulin signalling and attenuate glucose utilization. In fact, Arikawe et al.  revealed that high levels of fructose induce insulin resistance in rats. It has also been reported that prolonged high of fructose resulted in intracellular ATP depletion and uric acid generation. Subsequently, it may promote the development of renal injury . Further studies are necessary to clarify the possibility of metformin and vitexin in developing kidney complications.
In conclusion, this study demonstrated that F. deltoidea and vitexin had resulted in islets regeneration. These changes were accompanied by elevated pancreatic antioxidant enzymes. We essentially demonstrated that both functional and structural improvements of pancreas were also supported by composition of fatty acid and the pattern of FT-IR spectra. This raises the possibility of using F. deltoidea and vitexin as a valuable ancillary treatment that could add a novel layer of protection for the pancreas.
Fatty acids methyl esters
Fourier Transform Infrared
- GK :
Homeostasis assessment model of insulin resistance
Intraperitoneal glucose tolerance test
Intraperitoneal insulin tolerance test
Monounsaturated fatty acid
Peroxisome proliferator-activated receptor γ
Polyunsaturated fatty acids
Quantitative insulin sensitivity check index
Saturated fatty acid
Thiobarbituric acid reactive substances
- Tris- HCl:
Giacco F, Brownlee M, Schmidt AM. Oxidative stress and diabetic complications. Circ Res. 2010;107:1058–70. doi:10.1161/CIRCRESAHA.110.223545.
Forbes JM, Cooper ME. Mechanisms of diabetic complications. Physiol Rev. 2013;93:137–88. doi:10.1152/physrev.00045.2011.
Aronoff SL, Berkowitz K, Shreiner B, Want L. Glucose metabolism and regulation: beyond insulin and glucagon. Diabetes Spectrum. 2004;17(3):183–90. http://dx.doi.org/10.2337/diaspect.17.3.183.
Tiwari BK, Pandey KB, Abidi AB, Rizvi SI. Markers of oxidative stress during diabetes mellitus. J Biomark. 2013;2013:378790. doi:10.1155/2013/378790.
Couri CEB, Voltarelli JC. Potencial role of stem cell therapy in type 1 diabetes mellitus. Arq Bras Endocrinol Metabol. 2008;52(2):407–15. https://dx.doi.org/10.1590/S0004-27302008000200029.
Meier JJ, Bonadonna RC. Role of reduced β-cell mass versus impaired β-cell function in the pathogenesis of type 2 diabetes. Diabetes Care. 2013;2:S113–9. doi:10.2337/dcS13-2008.
Zhou JX, Dhawan S, Fu H, Snyder E, Bottino R, Kundu S, Kim SK, Bhushan A. Combined modulation of polycomb and trithorax genes rejuvenates β cell replication. J Clin Invest. 2013;123(11):4849–58. doi:10.1172/JCI69468.
Chen S, Bastarrachea RA, Roberts BJ, Voruganti VS, Frost PA, Nava-Gonzalez EJ, Arriaga-Cazares HE, Chen J, Huang P, DeFronzo RA, Comuzzie AG, Grayburn PA. Successful β cells islet regeneration in streptozotocin-induced diabetic baboons using ultrasound-targeted microbubble gene therapy with cyclinD2/CDK4/GLP1. Cell Cycle. 2014;13(7):1145–51. doi:10.4161/cc.27997.
Abdullah Z, Hussain K, Zhari I, Rasadah MA, Mazura P, Jamaludin F, Sahdan R. Evaluation of extracts of leaf of three Ficus Deltoidea varieties for antioxidant activities and secondary metabolites. Phcog Res. 2009;1:216–23.
Kalman DS, Schwartz HI, Feldman S, Krieger DR. Efficacy and safety of Elaeis guineensis and Ficus Deltoidea leaf extracts in adults with pre-diabetes. Nutr J. 2013;12:36. doi:10.1186/1475-2891-12-36.
Choo CY, Sulong NY, Man F, Wong TW. Vitexin and isovitexin from the leaves of Ficus Deltoidea with in-vivo α-glucosidase inhibition. J Ethnopharmacol. 2012;142(3):776–81. doi:10.1016/j.jep.2012.05.062.
Nurdiana S, Harita H, Farida Zuraina MY. Effect of Ficus Deltoidea leaves on glycolytic enzymes in liver of normal and streptozotocin-induced diabetic rats. Nat Prod. 2009;5(4):162–6.
Adam Z, Khamis S, Ismail A, Hamid M. Inhibitory properties of Ficus Deltoidea on α-glucosidase activity. Res J Med Plant. 2010;4:61–75. doi:10.3923/rjmp.2010.61.75.
Misbah H, Aziz AA, Aminudin N. Antidiabetic and antioxidant properties of Ficus Deltoidea fruit extracts and fractions. BMC Complement Altern Med. 2013;13(1):118. doi:10.1186/1472-6882-13-118.
Yao Y, Cheng X, Wang L, Wang S, Ren G. A determination of potential α-glucosidase inhibitors from Azuki beans (Vigna angularis). Int J Mol Sci. 2011;12(10):6445–51. doi:10.3390/ijms12106445.
Farsi E, Ahmad M, Hor SY, Ahamed MB, Yam MF, Asmawi MZ. Standardized extract of Ficus Deltoidea stimulates insulin secretion and blocks hepatic glucose production by regulating the expression of glucose-metabolic genes in streptozitocin-induced diabetic rats. BMC Complement Altern Med. 2014;14:220. doi:10.1186/1472-6882-14-220.
Ikeda T, Iwata K, Murakami H. Inhibitory effect of metformin on intestinal glucose absorption in the perfused rat intestine. Biochem Pharmacol. 2000;59(7):887–90. doi: https://doi.org/10.1016/S0006-2952(99)00396-2.
Zheng J, Woo SL, Hu X, Botchlett R, Chen L, Huo Y, Wu C. Metformin and metabolic diseases: a focus on hepatic aspects. Front Med. 2015;9(2):173–86. doi:10.1007/s11684-015-0384-0.
Jiang Y, Huang W, Wang J, Xu Z, He J, Lin X, Zhou Z, Zhang J. Metformin plays a dual role in MIN6 pancreatic β cell function through AMPK-dependent autophagy. Int J Biol Sci. 2014;10(3):268–77. doi:10.7150/ijbs.7929.
Motyl K, McCabe LR. Streptozotocin, type I diabetes severity and bone. Biol Proced Online. 2009;11:296–315.
Dong Y, Jing T, Meng Q, Liu C, Hu S, Ma Y, Liu Y, Lu J, Cheng Y, Wang D, Teng L. Studies on the antidiabetic activities of cordyceps militaris extract in diet-streptozotocin-induced diabetic Sprague-dawley rats. Biomed Res Int. 2014;2014:160980. doi:10.1155/2014/160980.
Tahara A, Matsuyama-Yokono A, Nakano R, Someya Y, Shibasaki M. Hypoglycaemic effects of antidiabetic drugs in streptozotocin-nicotinamide-induced mildly diabetic and streptozotocin-induced severely diabetic rats. Basic Clin Pharmacol Toxicol. 2008;103(6):560–8. doi:10.1111/j.1742-7843.2008.00321.x.
Abdollahi M, Zuki ABZ, Goh YM, Rezaeizadeh A, Noordin MM. The effects of Momordica charantia on the liver in streptozotocin-induced diabetes in neonatal rats. Afr J Biotechnol. 2010;9(31):5004–12.
Zhang C, Caldwell TA, Mirbolooki MR, Duong D, Park EJ, Chi NW, Chessler SD. Extracellular CADM1 interactions influence insulin secretion by rat and human islet β-cells and promote clustering of syntaxin-1. Am J Physiol Endocrinol Metab. 2016;310(11):E874–85. doi:10.1152/ajpendo.00318.2015.
Matthews DR, Hosker JP, Rudenski AS, Naylor BA, Treacher DF, Turner RC. Homeostasis model assessment: insulin resistance and beta-cell function from fasting plasma glucose and insulin concentrations in man. Diabetologia. 1985;28(7):412–9.
McAuley KA, Williams SM, Mann JI, Walker RJ, Lewis-Barned NJ, Temple LA, Duncan AW. Diagnosing insulin resistance in the general population. Diabetes Care. 2001;24(3):460–4. doi: https://doi.org/10.2337/diacare.24.3.460.
Lowry OH, Rosebrough NJ, Farr AL, Randall RJ. Protein measurement with the Folin phenol reagent. J Biol Chem. 1951;193(1):265–75.
Hardwick RN, Fisher CD, Canet MJ, Lake AD, Cherrington NJ. Diversity in antioxidant response enzymes in progressive stages of human nonalcoholic fatty liver disease. Drug Metab Dispos. 2010;38(12):2293–301. doi:10.1124/dmd.110.035006.
Eslami H, Batavani RA, Asr I-Rezaei S, Hobbenaghi R. Changes of stress oxidative enzymes in rat mammary tissue, blood and milk after experimental mastitis induced by E. coli lipopolysaccharide. Vet Res Forum. 2015;6(2):131–6.
Hajjar T, Goh YM, Rajion MA, Vidyadaran S, Li TA, Ebrahimi M. Alterations in neuronal morphology and synaptophysin expression in the rat brain as a result of changes in dietary n-6: n-3 fatty acid ratios. Lipids Health Dis. 2013;12:113. doi:10.1186/1476-511X-12-113.
Folch J, Lees M, Sloane Stanley GH. A simple method for the isolation and purification of total lipides from animal tissues. J Biol Chem. 1957;226(1):497–509.
Demir P, Akkas SB, Severcan M, Zorlu F, Severcan F. Ionizing radiation induces structural and functional damage on the molecules of rat brain homogenate membranes: a Fourier transform infrared (FT-IR) spectroscopic study. Appl Spectrosc. 2015;69(1):154–64. doi:10.1366/13-07154.
Petibois C, Déléris G, Piccinini M, Cestelli-Guidi M, Marcelli A. A bright future for synchrotron imaging. Nat Photonics. 2009;3:179. doi:10.1038/nphoton.2009.31.
Ordóñez P, Moreno M, Alonso A, Fernández R, Díaz F, González C. Insulin sensitivity in streptozotocin-induced diabetic rats treated with different doses of 17beta-oestradiol or progesterone. Exp Physiol. 2007;92(1):241–9. doi:10.1113/expphysiol.2006.035006.
Donga E, van Dijk M, Hoogma RP, Corssmit EP, Romijn JA. Insulin resistance in multiple tissues in patients with type 1 diabetes mellitus on long-term continuous subcutaneous insulin infusion therapy. Diabetes Metab Res Rev. 2013;29(1):33–8. doi:10.1002/dmrr.2343.
Subash-Babu P, Alshatwi AA, Ignacimuthu S. Beneficial antioxidative and antiperoxidative effect of Cinnamaldehyde protect streptozotocin-induced pancreatic β-cells damage in wistar rats. Biomol Ther (Seoul). 2014;22(1):47–54. doi:10.4062/biomolther.2013.100.
Ding Y, Zhang Z, Dai X, Jiang Y, Bao L, Li Y, Li Y. Grape seed proanthocyanidins ameliorate pancreatic beta-cell dysfunction and death in low-dose streptozotocin- and high-carbohydrate/high-fat diet-induced diabetic rats partially by regulating endoplasmic reticulum stress. Nutr Metab (Lond). 2013;10:51. 10.1186/1743-7075-10-51.
Amin A, Lotfy M, Mahmoud-Ghoneim D, Adeghate E, Al-Akhras MA, Al-Saadi M, Al-Rahmoun S, Hameed R. Pancreas-protective effects of chlorella in STZ-induced diabetic animal model: insights into the mechanism. J Diabetes Mellitus. 2011;1:36–45. doi:10.4236/jdm.2011.13006.
Abunasef SK, Amin HA, Abdel-Hamid GA. A histological and immunohistochemical study of beta cells in streptozotocin diabetic rats treated with caffeine. Folia Histochem Cytobiol. 2014;52(1):42–50. doi:10.5603/FHC.2014.0005.
Vetere A, Choudhary A, Burns SM, Wagner BK. Targeting the pancreatic β-cell to treat diabetes. Nat Rev Drug Discov. 2014;13(4):278–89. doi:10.1038/nrd4231. Epub 2014 Feb 14
Bhat M, Kothiwale SK, Tirmale AR, Bhargava SY, Joshi BN. Antidiabetic properties of Azardiracta indica and Bougainvillea spectabilis: in vivo studies in murine diabetes model. Evid Based Complement Alternat Med. 2011;2011:561625. doi:10.1093/ecam/nep033.
Hafizur RM, Fatima N, Shaukat S. Immunohistochemical evidence of pancreatic β-cell regeneration in streptozotocin-induced type 2 diabetic rats treated with Gymnema sylvestre extract. J Cytol Histol. 2015;6:342. doi:10.4172/2157-7099.1000342.
Oh YS. Plant-derived compounds targeting pancreatic beta cells for the treatment of diabetes. Evid Based Complement Alternat Med. 2015;2015:629863. 10.1155/2015/629863.
Roza AM, Pieper GM, Johnson CP, Adams MB. Pancreatic antioxidant enzyme activity in normoglycemic diabetic prone BB rats. Pancreas. 1995;10(1):53–8.
Gupta R, Sharma AK, Sharma MC, Gupta RS. Antioxidant activity and protection of pancreatic β-cells by embelin in streptozotocin-induced diabetes. J Diabetes. 2012;4(3):248–56. doi:10.1111/j.1753-0407.2012.00187.x.
Lei XG, Vatamaniuk MZ. Two tales of antioxidant enzymes on β cells and diabetes. Antioxid Redox Signal. 2011;14(3):489–503. doi:10.1089/ars.2010.3416.
Karunakaran U, Park KG. A systematic review of oxidative stress and safety of antioxidants in diabetes: focus on islets and their defense. Diabetes Metab J. 2013;37(2):106–12. doi:10.4093/dmj.2013.37.2.106.
Tiedge M, Lortz S, Drinkgern J, Lenzen S. Relation between antioxidant enzyme gene expression and antioxidative defense status of insulin-producing cells. Diabetes. 1997;46(11):1733–42. doi:10.2337/diab.46.11.1733.
Zhou QX, Liu F, Zhang JS, Lu JG, Gu ZL, Gu GX. Effects of triterpenic acid from Prunella vulgaris L. on glycemia and pancreas in rat model of streptozotozin diabetes. Chin Med J (Engl). 2013;126(9):1647-53.
Jurgens CA, Toukatly MN, Fligner CL, Udayasankar J, Subramanian SL, Zraika S, Aston-Mourney K, Carr DB, Westermark P, Westermark GT, Kahn SE, Hull RL. β-cell loss and β-cell apoptosis in human type 2 diabetes are related to islet amyloid deposition. Am J Pathol. 2011;178(6):2632–40. doi:10.1016/j.ajpath.2011.02.036.
Olsen JA, Kenna LA, Spelios MG, Hessner MJ, Akirav EM. Circulating differentially methylated amylin DNA as a biomarker of β-cell loss in type 1 diabetes. PLoS One. 2016;11(4):e0152662. doi:10.1371/journal.pone.0152662.
Pilkington EH, Gurzov EN, Kakinen A, Litwak SA, Stanley WJ, Davis TP, Ke PC. Pancreatic β-cell membrane fluidity and toxicity induced by human islet amyloid polypeptide species. Sci Rep. 2016;6:21274. doi:10.1038/srep21274.
Zhang S, Liu J, MacGibbon G, Dragunow M, Cooper GJ. Increased expression and activation of c-Jun contributes to human amylin-induced apoptosis in pancreatic islet beta-cells. J Mol Biol. 2002;324(2):271–85. doi:10.1016/S0022-2836(02)01044-6.
Cai K, Qi D, Wang O, Chen J, Liu X, Deng B, Qian L, Liu X, Le Y. TNF-alpha acutely upregulates amylin expression in murine pancreatic beta cells. Diabetologia. 2011;54(3):617–26. doi:10.1007/s00125-010-1972-9.
Shigihara N, Fukunaka A, Hara A, Komiya K, Honda A, Uchida T, Abe H, Toyofuku Y, Tamaki M, Ogihara T, Miyatsuka T, Hiddinga HJ, Sakagashira S, Koike M, Uchiyama Y, Yoshimori T, Eberhardt NL, Fujitani Y, Watada H. Human IAPP-induced pancreatic β cell toxicity and its regulation by autophagy. J Clin Invest. 2014;124(8):3634–44. doi:10.1172/JCI69866.
Fuentes AL, Hennessy K, Pascual J, Pepe N, Wang I, Santiago A, Chaggan C, Martinez J, Rivera E, Cota P, Cunha C, Nogaj LA, Moffet DA. Identification of plant extracts that inhibit the formation of diabetes-linked IAPP amyloid. J Herb Med. 2016;6(1):37–41.
Pithadia A, Brender JR, Fierke CA. Ramamoorthy: inhibition of IAPP aggregation and toxicity by natural products and derivatives. J Diabetes Res. 2016;2016:2046327. doi:10.1155/2016/2046327.
Bahramikia S, Yazdanparast R. Inhibition of human islet amyloid polypeptide or amylin aggregation by two manganese-salen derivatives. Eur J Pharmacol. 2013;707(1-3):17–25. doi:10.1016/j.ejphar.2013.03.017.
Cui W, Ma J, Wang X, Yang W, Zhang J, Ji Q. Free fatty acid induces endoplasmic reticulum stress and apoptosis of β-cells by Ca2+/calpain-2 pathways. PLoS One. 2013;8(3):e59921. doi:10.1371/journal.pone.0059921.
Němcová-Fürstová V, Balušíková K, Srámek J, James RF, Kovář J. Caspase-2 and JNK activated by saturated fatty acids are not involved in apoptosis induction but modulate ER stress in human pancreatic β-cells. Cell Physiol Biochem. 2013;31(2-3):277–89. doi:10.1159/000343367.
Martins EF, Miyasaka CK, Newsholme P, Curi R, Carpinelli AR. Changes of fatty acid composition in incubated rat pancreatic islets. Diabetes Metab. 2004;30(1):21–7. doi:10.1016/S1262-3636(07)70085-X.
Cnop M, Hannaert JC, Hoorens A, Eizirik DL, Pipeleers DG. Inverse relationship between cytotoxicity of free fatty acids in pancreatic islet cells and cellular triglyceride accumulation. Diabetes. 2001;50(8):1771–7. doi:10.2337/diabetes.50.8.1771.
Ahn JH, Kim MH, Kwon HJ, Choi SY, Kwon HY. Protective effects of oleic acid against palmitic acid-induced apoptosis in pancreatic AR42J cells and its mechanisms. Korean J Physiol Pharmacol. 2013;17(1):43–50. doi:10.4196/kjpp.2013.17.1.43.
Campillo JE, Luyckx AS, Torres MD, Lefebvre PJ. Effect of oleic acid on insulin secretion by the isolated perfused rat pancreas. Diabetologia. 1979;16(4):267–73. doi:10.1007/BF01221954.
Itoh Y, Kawamata Y, Harada M, Kobayashi M, Fujii R, Fukusumi S, Ogi K, Hosoya M, Tanaka Y, Uejima H, Tanaka H, Maruyama M, Satoh R, Okubo S, Kizawa H, Komatsu H, Matsumura F, Noguchi Y, Shinohara T, Hinuma S, Fujisawa Y, Fujino M. Free fatty acids regulate insulin secretion from pancreatic beta cells through GPR40. Nature. 2003;422(6928):173–6. doi:10.2337/diabetes.53.suppl_3.S16.
Vassiliou EK, Gonzalez A, Garcia C, Tadros JH, Chakraborty G, Toney JH. Oleic acid and peanut oil high in oleic acid reverse the inhibitory effect of insulin production of the inflammatory cytokine TNF-alpha both in vitro and in vivo systems. Lipids Health Dis. 2009;8:25. doi:10.1186/1476-511X-8-25.
Kudo T, Wu J, Ogawa Y, Suga S, Hasegawa N, Suda T, Mizukami H, Yagihashi S, Wakui M. Novel mechanism of chronic exposure of oleic acid-induced insulin release impairment in rat pancreatic beta-cells. J Pharmacol Exp Ther. 2006;318(3):1203–10. doi:10.1124/jpet.106.105759.
Zhang Y, Xiao M, Niu G, Tan H. Mechanisms of oleic acid deterioration in insulin secretion: role in the pathogenesis of type 2 diabetes. Life Sci. 2005;77(17):2071–81. doi:10.1016/j.lfs.2004.12.047.
Carrillo C, Del Mar CM, Roelofs H, Wanten G, Alonso-Torre SR. Activation of human neutrophils by oleic acid involves the production of reactive oxygen species and a rise in cytosolic calcium concentration: a comparison with N-6 polyunsaturated fatty acids. Cell Physiol Biochem. 2011;28(2):329–38. doi:10.1159/000331749.
Bellenger J, Bellenger S, Bataille A, Massey KA, Nicolaou A, Rialland M, Tessier C, Kang JX, Narce M. High pancreatic n-3 fatty acids prevent STZ-induced diabetes in fat-1 mice: inflammatory pathway inhibition. Diabetes. 2011;60(4):1090–9. doi:10.2337/db10-0901.
Hwang WM, Bak DH, Kim DH, Hong JY, Han SY, Park KY, Lim K, Lim DM, Kang JG. Omega-3 polyunsaturated fatty acids may attenuate streptozotocin-induced pancreatic β-cell death via autophagy activation in fat1 transgenic mice. Endocrinol Metab (Seoul). 2015;30(4):569–75. doi:10.3803/EnM.2015.30.4.569.
Baker MJ, Trevisan J, Bassan P, Bhargava R, Butler HJ, Dorling KM, Fielden PR, Fogarty SW, Fullwood NJ, Heys KA, Hughes C, Lasch P, Martin-Hirsch PL, Obinaju B, Sockalingum GD, Sulé-Suso J, Strong RJ, Walsh MJ, Wood BR, Gardner P, Martin FL. Using Fourier transform IR spectroscopy to analyze biological materials. Nat Protoc. 2014;9:1771–91. doi:10.1038/nprot.2014.110.
Sarre A, Gabrielli J, Vial G, Leverve XM, Assimacopoulos-Jeannet F. Reactive oxygen species are produced at low glucose and contribute to the activation of AMPK in insulin-secreting cells. Free Radic Biol Med. 2012;52(1):142–50. doi:10.1016/j.freeradbiomed.2011.10.437.
Kaung HC. Effect of glucose on beta cell proliferation and population size in organ culture of foetal and neonatal rat pancreases. J Embryol Exp Morphol. 1983;75:303–12.
Porat S, Weinberg-Corem N, Tornovsky-Babaey S, Schyr-Ben-Haroush R, Hija A, Stolovich-Rain M, Dadon D, Granot Z, Ben-Hur V, White P, Girard CA, Karni R, Kaestner KH, Ashcroft FM, Magnuson MA, Saada A, Grimsby J, Glaser B, Dor Y. Control of pancreatic β cell regeneration by glucose metabolism. Cell Metab. 2011;13(4):440–9. doi:10.1016/j.cmet.2011.02.012.
Pagliuca FW, Millman JR, Gürtler M, Segel M, Van Dervort A, Ryu JH, Peterson QP, Greiner D, Melton DA. Generation of functional human pancreatic β cells in vitro. Cell. 2014;159(2):428–39. doi:10.1016/j.cell.2014.09.040.
Assmann A, Ueki K, Winnay JN, Kadowaki T, Kulkarni RN. Glucose effects on beta-cell growth and survival require activation of insulin receptors and insulin receptor substrate 2. Mol Cell Biol. 2009;29(11):3219–28. doi:10.1128/MCB.01489-08.
Réus GZ, Dos Santos MA, Abelaira HM, Titus SE, Carlessi AS, Matias BI, Bruchchen L, Florentino D, Vieira A, Petronilho F, Ceretta LB, Zugno AI, Quevedo J. Antioxidant treatment ameliorates experimental diabetes-induced depressive-like behavior and reduces oxidative stress in brain and pancreas. Diabetes Metab Res Rev. 2016;32(3):278–88. doi:10.1002/dmrr.2732.
Bayeva M, Sawicki KT, Ardehali H. Taking diabetes to heart-deregulation of myocardial lipid metabolism in diabetic cardiomyopathy. J Am Heart Assoc. 2013;2(6):e000433. doi:10.1161/JAHA.113.000433.
Nolan CJ, Madiraju MS, Delghingaro-Augusto V, Peyot ML, Prentki M. Fatty acid signaling in the beta-cell and insulin secretion. Diabetes. 2006;55(Suppl 2):S16–23. doi:10.2337/db06-S003.
Chen YJ, Cheng YD, Liu HY, Lin PY, Wang CS. Observation of biochemical imaging changes in human pancreatic cancer tissue using Fourier-transform infrared microspectroscopy. Chang Gung Med J. 2006;29(5):518–27.
Sánchez-Lozada LG, Tapia E, Bautista-García P, Soto V, Avila-Casado C, Vega-Campos IP, Nakagawa T, Zhao L, Franco M, Johnson RJ. Effects of febuxostat on metabolic and renal alterations in rats with fructose-induced metabolic syndrome. Am J Physiol Renal Physiol. 2008;294(4):F710–8. doi:10.1152/ajprenal.00454.2007.
Jaiswal N, Maurya CK, Pandey J, Rai AK, Tamrakar AK. Fructose-induced ROS generation impairs glucose utilization in L6 skeletal muscle cells. Free Radic Res. 2015;49(9):1055–68. doi:10.3109/10715762.2015.1031662.
Arikawe AP, Udenze IC, Akinwolere MF, Ogunsola AO, Oghogholosu RT. Effects of streptozotocin, fructose and sucrose-induced insulin resistance on plasma and urinary electrolytes in male Sprague-Dawley rats. Nig Q J Hosp Med. 2012;22(4):224–30.
Johnson RJ, Nakagawa T, Jalal D, Sánchez-Lozada LG, Kang DH, Ritz E. Uric acid and chronic kidney disease: which is chasing which? Nephrol Dial Transplant. 2013;28(9):2221–8. doi:10.1093/ndt/gft029.
This research was supported by grants from the Ministry of Science, Technology and Innovation (SF: 100-RMI/SF 16/6/2 (7/2015), Ministry of Higher Education (MOE FRGS: 600-RMI/FRGS 5/3 (5/2014), Faculty of Applied Sciences, Universiti Teknologi MARA (UiTM) and Faculty of Veterinary Medicine, Universiti Putra Malaysia. We thank Laboratory Animal Facility and Management (LAFAM), UiTM for the postoperative care of the animals.
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All the data supporting analysis is contained within the manuscript.
NDS designed and carried out the studies, performed the statistical analysis, interpreted the results and drafted the manuscript. GYM supervised, designed the experiments and finalized the manuscript. NH, HA, DSM participated in biochemical analysis. NSA and NSNM carried out the animal handling and FT-IR work. EM performed the investigation of fatty acid changes and statistical analysis. All authors read and approved the final manuscript.
The authors declare that they have no competing interests.
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The study was approved by the Universiti Putra Malaysia, Animal Care and Use Committee with an approval number: UPM/IACUC/AUP-R090/2014.
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Nurdiana, S., Goh, Y.M., Ahmad, H. et al. Changes in pancreatic histology, insulin secretion and oxidative status in diabetic rats following treatment with Ficus deltoidea and vitexin. BMC Complement Altern Med 17, 290 (2017). https://doi.org/10.1186/s12906-017-1762-8
- F. deltoidea