Background
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 [
3]. 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 [
4]. It is thus justified to conclude that replenishment of insulin-producing pancreatic β-cells is crucial for treating diabetes and its complications [
5], 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 [
6]. 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 [
11].
F. deltoidea are known to be involved in lowering blood glucose level by enhancing the hepatic glycolytic enzymes in type 1 DM rats [
12]. 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. [
16] 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 [
19]. 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.
Methods
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 [
16]. 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.
Animals
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.) [
20]. After a week, animals with fasting blood glucose levels >11 mmol/L were considered diabetic [
21].
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) [
22], diabetic rats treated with 1000 mg/kg b.w. of
F.deltoidea (DFD) [
16], diabetic rats treated with 1 mg/kg b.w. of vitexin (DV) [
11].
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 [
23]. 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. [
24]. 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. [
25] while the quantitative insulin sensitivity check index (QUICKI) is based on the logarithmic transformation. Accordingly, McAuley’s index [
26] was calculated based on the increase of triglycerides levels and insulin according to the following equations:
$$ \mathrm{HOMA}-\mathrm{IR}=\frac{\mathrm{Fasting}\ \mathrm{insulin}\ \left(\frac{\upmu \mathrm{IU}}{\mathrm{mL}}\right)\times \mathrm{fasting}\ \mathrm{glucose}\ \left(\frac{\mathrm{mmol}}{\mathrm{L}}\right)}{22.5} $$
$$ \mathrm{HOMA}-\mathrm{B}=\frac{20\times \mathrm{Fasting}\ \mathrm{insulin}\ \left(\frac{\upmu \mathrm{IU}}{\mathrm{mL}}\right)\ }{\mathrm{fasting}\ \mathrm{glucose}\ \left(\frac{\mathrm{mmol}}{\mathrm{L}}\right)-3.5} $$
$$ \mathrm{QUICKI}=\frac{\ 1}{ \log fasting\ insulin\ \left(\frac{\mu IU}{mL}\right)+ \log fasting\ glucose\ \left(\frac{mg}{dL}\right)} $$
$$ \mathrm{McAuley}\ \mathrm{index}= \exp \left[2.63-0.28 \ln fasting\ insulin\ \left(\frac{\mu IU}{mL}\right)-0.31 \ln\ triglyceride\ \left(\frac{mmol}{L}\right)\right] $$
Histological assessment
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.
Fasting amylin
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 [
27], 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. [
28]. 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 [
29]. 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. [
30]. According to this method, 1 ml of serum were thawed at room temperature for 30 min and extracted using the Folch method [
31] (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 (BF
3) (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).
FT-IR analysis
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. [
32]. 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 [
33].
Statistical analysis
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.
Discussion
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 [
36]. 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 [
37]. 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 [
40]. Several plant extracts have been previously reported to be associated with the regeneration of pancreatic β-cells in STZ-treated diabetic rats [
41‐
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. [
48] 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. [
49] 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‐
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 [
53]. Cai et al. [
54] 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 [
55]. 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 [
58].
Disturbances of the fatty acid composition may be critical to explain the pancreatic β-cell destruction [
59]. 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 [
60]. In fact, a substantial increase in stearic acid content of pancreatic islets incubated in the presence of glucose had been previously reported [
61].
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. [
62] 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 [
63]. High concentrations of oleic acid have been pointed out to be effective in reversing the inhibitory effect in insulin production [
64‐
66]. Nevertheless, Kudo et al. [
67] 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 [
68] but enhanced the levels of intracellular free Ca
2+, which most likely accounts for the decrease of GSIS [
69].
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. [
70]. More details, Hwang et al. [
71] 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 [
72]. 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 [
73]. 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‐
76]. However, Assmann et al. [
77] 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. [
78]. Firmed convincing results have been published on the alterations of pancreatic structure and derangements in the lipid metabolism evoked by STZ [
79]. 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. [
80] 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 [
81].
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 [
82], thus, explains the reduction of FBG seen in the DM and DV groups. However, Jaiswal et al. [
83] 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. [
84] 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 [
85]. Further studies are necessary to clarify the possibility of metformin and vitexin in developing kidney complications.
Acknowledgement
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.