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Article

Chitin Extracted from the Shell of Blue Swimming Crabs (Portunus pelagicus Linn.) Inhibits NF-kappaB p65 in Ethanol-Induced Gastric Ulcerative Wistar Rats

by
Renny Amelia
1,*,
Sri Adi Sumiwi
2,
Nyi Mekar Saptarini
3 and
Jutti Levita
2,*
1
Department of Pharmacology, School of Pharmacy Muhammadiyah Cirebon, Cirebon 45153, West Java, Indonesia
2
Department of Pharmacology and Clinical Pharmacy, Padjadjaran University, Sumedang 45363, West Java, Indonesia
3
Department of Pharmaceutical Analysis and Medicinal Chemistry, Padjadjaran University, Sumedang 45363, West Java, Indonesia
*
Authors to whom correspondence should be addressed.
Mar. Drugs 2023, 21(9), 488; https://doi.org/10.3390/md21090488
Submission received: 25 July 2023 / Revised: 9 September 2023 / Accepted: 9 September 2023 / Published: 12 September 2023
(This article belongs to the Special Issue Poly- and Oligosaccharides from Marine Origins)
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Abstract

:
Peptic ulcer disease is generated by the activation of NF-kappaB activity. A recent clinical study reported a significant increase in NF-kappaB2 gene expression in 79 samples of peptic ulcer patients compared to the control group. Moreover, the deacetylated chitin could alter the translocation of NF-kappaB p65 to the nucleus. Considering this, our work aims to explore the effect of chitin extracted from the shell of blue swimming crabs (Portunus pelagicus Linn.) towards NF-kappaB p65 levels in ethanol-induced gastric ulcerative Wistar rats. The shells are found abundantly as the waste of seafood processing in the northern part of West Java, Indonesia. In this study, chitin extraction was carried out using the microwave-assisted extraction method by employing choline chloride (C5H14ClNO) and DL-malic acid (C₄H₆O₅) as the solvents. The inhibitory activity assay of chitin on the expression of NF-kappaB p65 was performed by using Western blot. The extraction yielded a good quality of chitin with a deacetylation degree of 30.8026%, molecular weight of 3.35 × 105 Da, and a negligible heavy metals level. Moreover, chitin extract at doses of 150, 300, and 600 mg/kg BW significantly reduced the percentage of gastric ulcer index compared to the negative control group. Meanwhile, chitin extract at doses of 300 and 600 mg/kg BW significantly inhibited NF-kappaB expression compared to the negative control group. Histopathological examination demonstrated a decrease in the number of necrotic cells and fat degeneration in the gastric mucosa and an increase in normal cells. Taken together, chitin extract obtained from the shells of blue swimming crabs may be able to prevent gastric ulcers induced by ethanol via the inhibition of NF-kappaB p65; however, further studies are needed to verify its anti-ulcerative properties.

1. Introduction

The activation of nuclear factor-kappaB (NF-kappaB) is governed by various mechanisms, e.g., interactions with its inhibitors. In the cell cytoplasm, NF-kappaB occurs in an inactive form as a complex with its inhibitor, IkappaB. Due to its capacity to stimulate the expression of various genes, the activity of NF-kappaB is firmly controlled at numerous stages [1,2,3]. NF-kappaB plays an important role as a mediator in the immune system. It contributes to stress responses and regulates cell proliferation and programmed cell death [3]. NF-kappaB is activated by proinflammatory factors such as interleukins and by Helicobacter pylori infection during the development of peptic ulcers. The NF-kappaB stimulation occurs when the IkappaB kinase complex is phosphorylated and eventually leads to the degradation of IkappaB. Inhibiting NF-kappaB leads to protection against long-term intestinal inflammation in animal models [4]. NF-kappaB was reported to be present in its active form in the healing phase of rats with gastric ulcers. Inflammatory cytokines, such as interleukin-1β, cyclooxygenase-2, and inducible nitric oxide synthase contribute to the development of gastric ulcers. Preventing the activation of NF-kappaB led to the recovery of gastric ulcers in rats [5]. Interestingly, a recent study in humans reported a significant increase in NF-kappaB2 gene expression in seventy-nine samples taken from patients diagnosed with peptic ulcers. However, no notable distinctions occurred in the expression of the NFKB2 gene between the patients infected and uninfected with H. pylori [6].
Chitin is a long-chain polymer of N-acetylglucosamine with β-(1–4) linkages, contained in the shell of crustaceans. It prevails in three isoforms, α-, β-, and γ-structures. The α-structure exists bountifully in nature [7]. A previous study reported that β-chitin had been successfully extracted from the exoskeleton of Portunus pelagicus Linn. [8]. During extraction, the shells of Crustaceans are reacted with an inorganic acid to dissolve calcium carbonate, followed by the addition of a strong base to remove protein [9].
Chitin has been reported for its activity in suppressing the production of proinflammatory interleukin-8 [7]. Different sizes of chitin also regulate the production of macrophage tumor necrosis factor (TNF) and IL-10 in C57BL/6 mice [10]. Chitin can upregulate and downregulate the effect of the NLR family pyrin domain containing 3 (NLRP3) inflammasomes based on its preparation [11]. Deacetylated chitin altered the translocation of NF-kappaB p65 to the nucleus as proven by the significant decrease of the mRNA expression of p65 under heat stress compared to the negative control group (p < 0.05) [12]. Chitin extracted from shrimp and squilla shell waste was reported to exhibit antioxidant activity and inhibit the growth of Staphylococcus aureus and Escherichia coli [13].
In the northern part of West Java, Indonesia, blue swimming crab shells are present lavishly as waste from the processing of seafood. Up to a point, these shells have not been utilized for their health and economic values; accordingly, our work aims to explore whether chitin contained in these shells possesses an anti-inflammatory activity via the inhibition of NF-kappaB p65 in ethanol-induced gastric ulcerative Wistar rats.

2. Results

2.1. The Taxonomy Identification of the Crab Shells and the Physicochemical Properties of the Crab Shell Powder and the Chitin Extract

The fresh blue swimming crab shells (Figure 1) were identified at the Zoology Museum-Laboratory of Identification and Determination, School of Life Sciences and Technology, Bandung Institute of Technology, and based on characteristics described by Poore (2004) [14], Lai et al. (2010) [15], were confirmed as Portunus pelagicus Linn. (No. 2974/11.C02.2/2019).
The physicochemical properties of the crab shell powder and the chitin extract, respectively, were as follows: the water content was 4.53% and 0.88%, protein was 8.17% and 6.30%, lipid was 0.26% and 0.28%, and carbohydrate was 15.73% and 55.86.
The levels of five toxic heavy metals of the crab shell powder and the chitin extract, respectively, were as follows: mercury was 5.73 ± 0.005 mg/kg and <0.0001 mg/kg, lead was 3.46 ± 0.24 and <0.0001 mg/kg, chromium was 2.55 ± 0.00 mg/kg and 13.09 ± 0.02 mg/kg, cadmium was 0.29 ± 0.00 mg/kg and <0.0001 mg/kg, and arsenic was 64.16 ± 2.67 mg/kg and <0.0001 mg/kg.
FT-IR spectrum of chitin extract (depicted in Figure 2) demonstrated the amide C=O band at 1620.41 cm−1 (%T value of 19.805% or A = −1.2967) and the OH stretch band at 3434.64 cm−1 (%T value of 26.441% or A = −1.4222). Thus, the deacetylation degree (DD) of chitin extract, determined by calculating the absorbance of these bands, was 30.8026%.
The intrinsic viscosity (η) of chitin 1% solution in acetic acid at 27.3 °C was 1.9750 ± 0.031 centipoise (cP). By using the Mark–Houwink equation, the molecular weight of chitin was obtained at 3.35 × 105 Da.

2.2. Effect of Chitin Extract, Commercial Chitin, and Shell Powder on the % Relative Organ Weight and % Ulcer Index

The results of hematoxylin-eosin (HE) staining are depicted in Figure 3.
All doses of chitin extract, commercial chitin, and crude shell powder demonstrate significant differences in % ulcer index compared to the negative control group. The effect exhibited by chitin extract, commercial chitin, and crude shell powder is similar to the rats treated with sucralfate (the positive control group) (Table 1). There is no significant difference in the % relative organ weight of all treated rat groups compared to the negative control group (Table 1).

2.3. Effect of Different Doses of Chitin Extract, Commercial Chitin, and Shell Powder on the Hemorrhagic Severity of the Gastric Mucosa in Ethanol-Induced Gastric Ulceration Rats

Inducing rats with ethanol (5 mL/kg BW, orally by intragastric gavage) caused a severe gastric lesion (Figure 4 and Table 2). The pretreatment with sucralfate, the control drug (1080 mg/kg BW, orally), could protect the stomach against ethanol-induced gastric mucosa hemorrhage. Similarly, higher doses of chitins in the form of extracts, commercials, and crude shell powders could reduce the severity of ethanol-induced damage (Figure 4). Nonetheless, pretreatment using lower concentrations of chitin extract (150 mg/kg BW) resulted in only weak protection.

2.4. Effect of Different Doses of Chitin Extract, Commercial Chitin, and Shell Powder on the Expression of NF-kappaB p65 in Western Blot Analysis

Figure 5 shows the bands of NF-kappaB p65 (molecular weight of 65 kDa) and β-actin (molecular weight of 42 kDa) in the stomach of the Wistar rats, respectively. Chitin extracts (dose of 300 mg/kg BW and 600 mg/kg BW), all doses of commercial chitin, and crude shell powder dose of 500 mg/kg BW could significantly reduce the expression of NF-kappaB p65 in the stomach of ethanol-induced gastric ulcerative rats. The inhibitory activity on NF-kappaB p65 expression by chitin extracts is better than that of sucralfate (the positive control drug). However, an increase in the relative expression of NF-kappaB p65 was observed at the lowest dose of chitin extract (150 mg/kg BW) and the highest dose of crude shell powder (1000 mg/kg BW).

3. Discussion

The main findings of our work are (1) chitin extracted from the shells of blue swimming crabs at doses of 150, 300, and 600 mg/kg BW significantly reduced the percentage of gastric ulcer index in ethanol-induced gastric ulcerative rats; (2) chitin extract at doses of 300 and 600 mg/kg BW significantly inhibited NF-kappaB levels compared to the negative control group.
It was confirmed that excessive alcohol drinking had demonstrated damage to the gastrointestinal tract. A previous prospective study on 48,000 males aged 40–75 years reported that those who consumed >30 g/day of alcohol exhibited a notable risk for major gastric bleeding when compared to non-alcohol drinkers [16]. Studies on the endoscopic examination of thousands of patients with peptic ulcers confirmed that there was a correlation between this disease and the risk factors, among which is alcohol consumption [17,18]. These studies have been the reason why ethanol was chosen for the gastric-ulcerative inducer in our study.
Based on its source, chitin in nature presents in two structures, α-chitin, which is the most abundant, and β-chitin [19]. Numerous studies reported the source of chitin extraction, e.g., from the exoskeletons of prawns [20], shrimps [21,22,23,24], and crabs [8,12,25,26].
In the present study, chitin extracted from the shells of blue swimming crabs was assayed for its water (0.88%), protein (6.30%), lipid (0.28%), and carbohydrate (55.86) contents. Chitin extract was confirmed safe as proven by the low levels of five toxic heavy metals (mercury < 0.0001 mg/kg, lead < 0.0001 mg/kg, chromium 13.09 ± 0.02 mg/kg, cadmium < 0.0001 mg/kg, and arsenic < 0.0001 mg/kg). The deacetylation degree (DD) of the extract was 30.8026% and the molecular weight was 3.35 × 105 Da, which further proved the presence of chitin and the quality of the extract.
A deacetylation degree (DD) value of <60% indicates the presence of chitin, whereas a DD of >60% belongs to chitosan [27,28]. It was reported that the DD value of chitin obtained from mud crab shells collected in Brunei Darussalam was 48.0% [29]. Another FTIR analysis on chitin extracted from Labeo rohita fish collected in Rourkela, India revealed a DD value of 61% [30]. Moreover, the DD value of chitin extracted from the shrimp waste collected in a local fish market of Buraidah, Qassim, Kingdom of Saudi Arabia was 70.9% at pH 8.4 [31].
Meanwhile, the present study revealed that pretreatment with chitin could protect the gastric mucosal cells against ethanol-induced ulcerative damage. It seems that the gastroprotective activity of chitin also advances the immune system. A previously reported clinical trial on 24 volunteers confirmed chitin activates the immune system [32], by inducing the production of type 1 cytokines, thus preventing type 2 inflammation [33]. It was reported chitin could activate T cells and natural killer cells, and stimulate the synthesis of interferon-γ [34].
In our study, chitin extracts could significantly reduce the expression of NF-kappaB p65 in the stomach of ethanol-induced gastric ulcerative rats. Although there is a very limited report on the inhibitory activity of chitin against NF-kappaB, a recent study confirmed that the deacetylated form of chitin in nanoparticles significantly reduced mRNA gene expression of GSK-3, TNF-α, and NF-kappaB. NF-kappaB is activated through oxidative stress, which eventually induces an inflammatory cascade by initiating the gene transcription of many proinflammatory cytokines [35].
Moreover, the ulcer healing process requires several biological and molecular reactions, including inflammatory response and cell migration. Therapeutic strategy for inflammatory diseases aims to block NF-kappaB activity in several mechanisms, (1) by inhibiting IKK activity; (2) by suppressing protease activity; (3) by inhibiting the translocation of NF-kappaB to the nucleus; thus, the NF-kappaB subunits such as RelA (p65), p50, c-Rel, and other NF-kappaB subunits will be prevented from entering the nucleus; and (4) by preventing the binding of NF-kappaB subunits with DNA [36]. However, a dose of 300 mg/kg BW of purified chitosan, the deacetylated derivative of chitin, demonstrated an anti-inflammatory activity on mice infected with enterotoxigenic Escherichia coli [37]. A dose of 16 mg/kg BW of purified chitin oligosaccharide was reported to reduce inflammation on ovalbumin (OVA)-induced lung inflammation in a mouse model of asthma [38]. A dose of 10 mg/kg BW of pure chitosan (purity 98%) decreased the AST, ALT, and ALP, and improved the histology of CCl4-induced hepatic fibrosis (HF) rat models [39].
Our study confirms that chitin alleviates peptic ulcers by inhibiting the translocation of the NF-kappaB p65 subunit to the nucleus, as shown by the disappearance of the NF-kappaB p65 bands in the Western blot electropherogram (Figure 5). Similarly, it was reported in a previous study that chitin extracted from cuttlebone was able to heal wound lesions in rat models. Cuttlebone chitin can stimulate macrophages and increase the expression of TNF-α, IL-1β, and IL-6. Increased production of IL-8 also occurs due to fibroblast migration, thereby accelerating the wound-healing process [7].
Chitin activates cytokine production, leukocyte recruitment, and macrophage activation. It is sensed by the immune system via specific membrane-bound receptors and is important in defense against pathogens [40].
However, the limitation of our study is lacking the data on IL-6 expression. IL-6 is a biomarker for gastric inflammation [41], thus opening the chance for future studies that an evaluation of another NF-kappaB such as IL-6, GSK-3, and TNF-α can be carried out.

4. Materials and Methods

4.1. Chemicals and Antibodies

Choline chloride (Salus Nutra Inc., Xian, China), DL-malic acid (Salus Nutra Inc., Xian, China), commercial chitin (Carbosynth, China), sucralfate (Combiphar, Bandung, Indonesia), ethanol, pure 99.5% (Merck Millipore-Sigma Aldrich, USA), ethyl ether (Merck Millipore-Sigma Aldrich, St. Louis, MI, USA), carboxymethyl cellulose (CMC) (BrataChem, Bandung, Indonesia), Bouin solution, distilled water (BrataChem, Bandung, Indonesia), mouse monoclonal IgG1 NF-kappaB p65 antibody (Santacruz Biotechnology Inc., K2320, Shanghai, China), β-actin antibody (Thermo Scientific MA5-15739, Singapore), anti-mouse antibody (Li-Cor C90408-07, PT. Elo Karsa Utama, Jakarta, Indonesia), bovine serum albumin (BSA Protein, Thermo Scientific, Singapore), sodium dodecyl sulfate (SDS) gel 15% (Merck Millipore-Sigma Aldrich, St. Louis, MI, USA), polyvinylidene difluoride (PVDF) membrane (Merck Millipore-Sigma Aldrich, St. Louis, MI, USA), phosphate buffer saline-tween 20 (PBST) 0.1%, protein ladder (Thermo Scientific, Singapore), running buffer, transfer buffer, lysis buffer.

4.2. Crab Shells

Fresh blue swimming crab shells were collected in a traditional market in Gunung Jati Cirebon, the northern part of West Java, with size ranges of 13–15 cm. The shells were boiled, washed meticulously to remove meat residue and dirt, and sun-dried for three days. The dried shells were ground to powder and sieved using a sieve mesh-60. The powder was put in sealed plastic pouches with silica gels until further processed.

4.3. Extraction of Chitin and Analysis of the Physicochemical Properties

The extraction of chitin was carried out following a previous study employing a microwave-assisted extraction method [8]. The blue swimming crab shell powder was dissolved in a mixture of 69.8 g of choline chloride (C5H14ClNO; molecular weight of 139.62) and 67.045 g of DL-malic acid (C4H6O5; molecular weight of 134.09) in 1 L of distilled water. The mixture was stirred at 80 °C until homogenous, then was put in a microwave (Rewez Multifunctional) at 700 watts for 9 min, and every minute it was taken out for three seconds to prevent overheating. Chitin, yielded as precipitate, was separated from the solvent by centrifugation (80-1 tabletop low-speed centrifuge), washed using distilled water, and the extraction was repeated 2×. This extraction technique yielded 35.43% w/w of yellowish-white chitin precipitate.
The physicochemical properties, in terms of the water content (gravimetric method), protein (Kjeldahl method), lipid (Soxhlet method), and carbohydrate (by difference method) in the extract were determined by following the Indonesian Standardization Agency (1992) Methods for Analyzing Food and Beverages (SNI 01-2891-1992) [42]. The levels of five toxic heavy metals (mercury at 253.6 nm, lead at 220.4 nm, chromium at 283.6 nm, cadmium at 226.5 nm, and arsenic at 188.9 nm) were also analyzed using an Inductively Coupled Plasma Optical Emission spectroscopy (Agilent Technologies 725). These works were done at the Central Laboratory, Directorate of Research and Community Engagement, Padjadjaran University, in October 2020.
The deacetylation degree (DD) of chitin extract was (1) determined by Fourier Transform-Infrared spectrometer, which is based on the absorbance (A) ratio of the amide band of the acetyl group at 1650 cm−1 and the OH (hydroxyl) group band at 3450 cm−1 by following the equation of [27,28,29]:
DD (%) = 100 − 75.19 [A1650/A3450]
The chitin-potassium bromide pellets were prepared by dispersing 1 mg of dry chitin extract powder in 200 mg of potassium bromide and were compressed under a vacuum for 10 min to obtain the potassium bromide discs. The discs were recorded in an FT-IR spectrometer (NicoletTM 380 FT-IR ThermoFisher Scientific) at a frequency range of 4000–500 cm−1.
The molecular weight (MW) of chitin was calculated by determining the viscosity of 1% chitin solution in acetic acid. The solution was stirred for 4 h, measured in an Ostwald viscometer, and the viscosity was calculated by following an equation of Mark–Houwink [43]:
[η] = KMa or Log [η] = Log K + a (Log M)
where η = intrinsic viscosity (in centipoise, cP), K = 1.74 × 10−5 L/g and a (the slope), both of which are constants depending on the DD of chitin; and M = molecular weight.

4.4. Animals and Ethical Considerations

Forty-four male Wistar rats, 10–12 weeks, 190–210 g were used in this study. The number of animals used was calculated using the Federer Formula: (12 − 1) × (n − 1) ≥ 15, which resulted in n = 4 for each group, but only data from 3 animals in each group were included. No animals were found dead during the study (the duration of the study was 40 days). Rat handling and euthanasia procedures were performed as approved by the Research Ethics Committee, Padjadjaran University, Indonesia, recognized by the Forum of Ethics Review Committee in Asia & Western Pacific Region (approval document No. 541/UN6. KEP/EC/2020).

4.5. Animal Preparation and Treatment Groups

The in vivo experiment was carried out in the Pharmacology Laboratory, School of Pharmacy Muhammadiyah Cirebon, West Java. The design of the study strictly followed Essential 10 of the ARRIVE guidelines (Animal Research: Reporting of In Vivo Experiments) [44]: Forty-four male Wistar rats were randomly assigned into 11 groups (n = 4) and treated for 13 consecutive days. The rats were kept in animal cages (cage base area 148 cm2, cage height 20 cm) at 24–26 °C under a 12 h light, 12 h dark cycle, and were provided with standard pellet food (Citra Feed RatBio) 150 g/cage daily and water freely for 7 days. Animal health and behavior were observed daily. The cages were cleaned every 2 days:
  • Group 1: positive control, treated with sucralfate (1080 mg/kg BW);
  • Group 2: negative control or placebo, treated with CMC 1% suspension;
  • Group 3: normal control, without any treatment;
  • Group 4: treated with chitin extract (dose of 150 mg/kg BW);
  • Group 5: treated with chitin extract (dose of 300 mg/kg BW);
  • Group 6: treated with chitin extract (dose of 600 mg/kg BW);
  • Group 7: treated with commercial chitin (dose of 150 mg/kg BW);
  • Group 8: treated with commercial chitin (dose of 300 mg/kg BW);
  • Group 9: treated with commercial chitin (dose of 600 mg/kg BW);
  • Group 10: treated with crab shell powder (dose of 500 mg/kg BW);
  • Group 11: treated with crab shell powder (dose of 1000 mg/kg BW).
On day 14 before the initiation of gastric ulcer, the rats were not given feed for 12 h to establish an empty stomach (the drink was still given freely).

4.6. Induction of Ulcer

The initiation of ulcers in all rats, except the normal group, was performed by orally administering absolute ethanol at a dose of 5 mL/kg BW using an intragastric feeder, as delineated previously [45]. The optimization of the ethanol-ulcerative inducing time before the animal sacrifice was determined as follows using a total of 4 rats for each different time: 30 min; 1 h; 1.5 h; 2 h. None of the rats died prematurely prior to euthanasia. The death was verified with the absence of pupillary to direct and consensual light, pupils not equal or dilated, failure of the heart rate, and absence of respiratory efforts. The result is depicted in Figure 6. Based on this result, the inducing time of 1 h was chosen, because the severity of the hemorrhagic area is not as large compared to the inducing time of 1.5 h and 2 h.

4.7. Relative Organ Weight

The rats were anesthetized using ether inhalation and sacrificed, 1 h after ulcer induction by cervical dislocation, and the stomach of all groups was separated, cleansed with 0.9% sodium chloride in water, macroscopically examined, and weighed. The relative stomach weight was calculated as follows:
%   R e l a t i v e   s t o m a c h   w e i g h t = s t o m a c h   w e i g h t b o d y   w e i g h t × 100 %

4.8. Histopathological Examination of the Stomach

The clean stomach of all groups was sectioned at the major curvature for histological studies. The stomach was fixed in a 10% Bouin solution. The Bouin-fixed stomach sections were embedded in paraffin wax, subsequently sliced to 2–3 μm thickness, stained with hematoxylin with 15 min soaking time and eosin with 4 min soaking time at room temperature (H&E), and perceived for pathologic diversities using an Olympus CX33 microscope, and the ulcer area was measured using ImageJ software. Ulcer index (%) was calculated as follows:
% Ulcer index = [ulcer area/total area of stomach mucosa] × 100%

4.9. Effect of Chitin towards the Infiltration of Inflammatory Cells

The infiltration of inflammatory cells on the gastric mucosa was observed using a light microscope with a magnification of 400× and 1000× to count the number of normal cells, necrotic cells, and fat degeneration.

4.10. Effect of Chitin towards NF-kappaB p65 in Ethanol-Induced Gastric Ulcerative Wistar Rats

The rats’ 2–3 μm thickness of stomach tissue was homogenized in a lysis buffer. The protein samples were heat-denatured at 95 °C for 5 min and cooled to room temperature. Samples (10–15 μg/lane) were separated by sodium dodecyl sulfate-polyacrylamide gel electrophoresis (SDS-PAGE) at an initial voltage of 80 V, followed by gradually increasing the voltage from 80 V, 100 V, 120 V, to 150 V for 1 h, conveyed to a nitrocellulose membrane (GE Healthcare) for 1 h at 20–22 °C, and occluded for twelve hours at 4 °C in Tris-buffered saline with 0.1% Tween® 20. Immunoblotting was performed using a mouse monoclonal NF-kappaB p65 antibody (Santacruz Biotechnology Inc., diluted 1:100 in bovine serum albumin 0.2%). Blots were stripped, cleansed with phosphate-buffered saline Tween20 0.1% detergent (PBST) three times, and re-probed using a secondary antibody (anti-mouse monoclonal antibody in bovine serum albumin 0.2%) as the internal control, incubated for 2 h, and washed with PBST 0.1% three times. The signals were developed using an enhanced chemiluminescence reagent (GE Healthcare), scanned using LI-COR Odyssey scanner, and the intensity of the band was measured using ImageJ-Win64 (https://imagej.nih.gov/ij/ accessed on 31 May 2021).

4.11. Statistical Analysis

Data were analyzed using IBM SPSS Statistics version 24.0. Normally distributed data were analyzed using the One-way ANOVA, further analysis was performed with a post hoc test using LSD, and other data were analyzed using Mann-Whitney. p-value < 0.05 indicates a statistical significance. The experiments were performed in triplicates.

5. Conclusions

Chitin was successfully extracted from the shells of blue swimming crabs (Portunus pelagicus Linn.) using a mixture of choline chloride and DL-malic acid as the solvent. The physicochemical properties of the chitin extract confirmed its good quality. Chitin extract could protect the gastric mucosal cells against ethanol-induced ulcerative damage. It seems that the gastroprotective activity of chitin also advances the immune system by decreasing the expression of NF-kappaB p65 in the rats’ stomachs, thereby preventing the protein from translocating to the nucleus. Ultimately, the inflammatory process will not take place. Taking everything into consideration, chitin extracted from the shells of blue swimming crabs might be able to prevent gastric ulcers via the inhibition of NF-kappaB p65, thus confirming the health values of these seafood wastes. However, further studies are needed to verify its anti-ulcerative properties.

Author Contributions

Conceptualization, J.L. and S.A.S.; methodology, J.L., S.A.S. and N.M.S.; formal analysis, R.A.; investigation, R.A.; resources, S.A.S.; validation of raw data, J.L. and N.M.S.; writing—original draft preparation, R.A.; writing—review and editing, J.L. and R.A.; supervision, J.L., S.A.S. and N.M.S. All authors have read and agreed to the published version of the manuscript.

Funding

This research (Academic-Leadership Research Grant No. 1959/UN6.3.1/PT.00/2020 and 1959/UN6.3.1/PT.00/2021) and the APC are funded by the Rector of Padjadjaran University via the Directorate of Research and Community Engagement.

Institutional Review Board Statement

The animal study protocol was approved by the Research Ethics Committee, Padjadjaran University, Indonesia, recognized by the Forum of Ethics Review Committee in Asia & Western Pacific Region (approval document No. 541/UN6. KEP/EC/2020).

Data Availability Statement

Not applicable.

Acknowledgments

The authors thank (1) the Head of the Central Laboratory, Directorate of Research and Community Engagement, Padjadjaran University for providing the instruments and the analytical support; (2) the Head of the Pharmacology Laboratory, Faculty of Pharmacy, Padjadjaran University; and (3) the Head of Pharmacology Laboratory, School of Pharmacy Muhammadiyah Cirebon for the continuous facilitation and animal handling support.

Conflicts of Interest

The authors declare no conflict of interest.

References

  1. Hoesel, B.; Schmid, J.A. The Complexity of NF-κB Signaling in Inflammation and Cancer. Mol. Cancer 2013, 12, 86. [Google Scholar] [CrossRef] [PubMed]
  2. Guo, X.; Koff, J.L.; Moffitt, A.B.; Cinar, M.; Ramachandiran, S.; Chen, Z.; Switchenko, J.M.; Mosunjac, M.; Neill, S.G.; Mann, K.P.; et al. Molecular Impact of Selective NFKB1 and NFKB2 Signaling on DLBCL Phenotype. Oncogene 2017, 36, 4224–4232. [Google Scholar] [CrossRef] [PubMed]
  3. Oeckinghaus, A.; Ghosh, S. The NF-kappaB Family of Transcription Factors and Its Regulation. Cold Spring Harb. Perspect. Biol. 2009, 1, a000034. [Google Scholar] [CrossRef]
  4. Spehlmann, M.E.; Eckmann, L. Nuclear Factor-kappa B in Intestinal Protection and Destruction. Curr. Opin. Gastroenterol. 2009, 25, 92–99. [Google Scholar] [CrossRef]
  5. Takahashi, S.; Fujita, T.; Yamamoto, A. Role of Nuclear Factor-kappaB in Gastric Ulcer Healing in Rats. Am. J. Physiol. Gastrointest. Liver Physiol. 2001, 280, G1296–G1304. [Google Scholar] [CrossRef] [PubMed]
  6. Marta, Ż.-N.; Agnieszka, W.; Jacek, P.; Jeleń, A.; Adrian, K.; Dagmara, S.; Sałagacka-Kubiak, A.; Balcerczak, E. NFKB2 Gene Expression in Patients with Peptic Ulcer Diseases and Gastric Cancer. Mol. Biol. Rep. 2020, 47, 2015–2021. [Google Scholar] [CrossRef]
  7. Lim, S.C.; Lee, K.M.; Kang, T.J. Chitin from Cuttlebone Activates Inflammatory Cells to Enhance the Cell Migration. Biomol. Ther. 2015, 23, 333–338. [Google Scholar] [CrossRef] [PubMed]
  8. Amelia, R.; Indawati, I.; Saptarini, N.M.; Sumiwi, S.A.; Levita, J. The Proximate Analysis and Spectral Profile of Chitin Extracted from the Shell of Portunus pelagicus Originated from Cirebon, Indonesia. Rasayan J. Chem. 2021, 14, 1755–1760. [Google Scholar] [CrossRef]
  9. Badwan, A.A.; Rashid, I.; Omari, M.M.H.A.; Darras, F.H. Chitin and Chitosan as Direct Compression Excipients in Pharmaceutical Applications. Mar. Drugs 2015, 13, 1519–1547. [Google Scholar] [CrossRef]
  10. Da Silva, C.A.; Chalouni, C.; Williams, A.; Hartl, D.; Lee, C.G.; Elias, J.A. Chitin is a Size-dependent Regulator of Macrophage TNF and IL-10 Production. J. Immunol. 2009, 182, 3573–3582. [Google Scholar] [CrossRef]
  11. Dhanjal, C.R.; Lingamsetty, R.; Pareddy, A.; Kim, S.-K.; Raval, R. Dual Role of Chitin as the Double-edged Sword in Controlling the NLRP3 Inflammasome Driven Gastrointestinal and Gynaecological Tumours. Mar. Drugs 2022, 20, 452. [Google Scholar] [CrossRef] [PubMed]
  12. Mohyuddin, S.G.; Qamar, A.; Hu, C.Y.; Chen, S.W.; Wen, J.Y.; Liu, X.X.; Ma, X.B.; Yu, Z.C.; Yong, Y.H.; Wu, L.Y.; et al. Effect of Chitosan on Blood Profile, Inflammatory Cytokines by Activating TLR4/NF-κB Signaling Pathway in Intestine of Heat-Stressed Mice. Sci. Rep. 2021, 11, 20608. [Google Scholar] [CrossRef] [PubMed]
  13. Limam, Z.; Selmi, S.; Sadok, S.; El Abed, A. Extraction and Characterization of Chitin and Chitosan from Crustacean By-products: Biological and Physicochemical Properties. Afr. J. Biotechnol. 2011, 10, 640–647. [Google Scholar]
  14. Poore, G.C.B. Marine Decapod Crustacea of Southern Australia a Guide to Identification with a Chapter on Stomatopoda by Shane Ahyong; CSIRO Publishing: Clayton, Australia, 2004; pp. 215–240. [Google Scholar]
  15. Lai, J.C.Y.; Ng, P.K.L.; Davie, P.J.F. A revision of the Portunus pelagicus (Linnaeus, 1758) species complex (Crustacea: Brachyura: Portunidae), with the recognition of four species. Raffles Bull. Zool. 2010, 58, 199–237. [Google Scholar]
  16. Strate, L.L.; Singh, P.; Boylan, M.R.; Piawah, S.; Cao, Y.; Chan, A.T. A Prospective Study of Alcohol Consumption and Smoking and the Risk of Major Gastrointestinal Bleeding in Men. PLoS ONE 2016, 11, e0165278. [Google Scholar] [CrossRef]
  17. Kang, J.W.; Lee, J.S.; Bae, K.M. Correlation between Peptic Ulcer Disease and Risk Factors. Korean J. Fam. Pract. 2016, 6, 479–483. [Google Scholar] [CrossRef]
  18. Lee, S.P.; Sung, I.-K.; Kim, J.H.; Lee, S.-Y.; Park, H.S.; Shim, C.S. Risk Factors for the Presence of Symptoms in Peptic Ulcer Disease. Clin. Endosc. 2017, 50, 578–584. [Google Scholar] [CrossRef]
  19. Younes, I.; Rinaudo, M. Chitin and Chitosan Preparation from Marine Sources. Structure, Properties and Applications. Mar. Drugs 2015, 13, 1133–1174. [Google Scholar] [CrossRef]
  20. Tan, Y.N.; Lee, P.P.; Chen, W.N. Microbial Extraction of Chitin from Seafood Waste Using Sugars Derived from Fruit Waste-Stream. AMB Express 2020, 10, 17. [Google Scholar] [CrossRef]
  21. Percot, A.; Viton, C.; Domard, A. Optimization of Chitin Extraction from Shrimp Shells. Biomacromolecules 2003, 4, 12–18. [Google Scholar] [CrossRef]
  22. Xie, J.; Xie, W.; Yu, J.; Xin, R.; Shi, Z.; Song, L.; Yang, X. Extraction of Chitin from Shrimp Shell by Successive Two-step Fermentation of Exiguobacterium profundum and Lactobacillus acidophilus. Front. Microbiol. 2021, 12, 677126. [Google Scholar] [CrossRef] [PubMed]
  23. Doan, C.T.; Tran, T.N.; Nguyen, V.B.; Vo, T.P.K.; Nguyen, A.D.; Wang, S.-L. Chitin Extraction from Shrimp Waste by Liquid Fermentation Using an Alkaline Protease-Producing Strain, Brevibacillus parabrevis. Int. J. Biol. Macromol. 2019, 131, 706–715. [Google Scholar] [CrossRef] [PubMed]
  24. Benhabiles, M.S.; Salah, R.; Lounici, H.; Drouiche, N.; Goosen, M.F.A.; Mameri, N. Antibacterial activity of chitin, chitosan and its oligomers prepared from shrimp shell waste. Food Hydrocoll. 2012, 29, 48–56. [Google Scholar] [CrossRef]
  25. Huang, W.C.; Zhao, D.; Xue, C.; Mao, X. An Efficient Method for Chitin Production from Crab Shells by a Natural Deep Eutectic Solvent. Mar. Life Sci. Technol. 2022, 4, 384–388. [Google Scholar] [CrossRef]
  26. Kaya, M.; Baran, T.; Karaarslan, M. A New Method for Fast Chitin Extraction from Shells of Crab, Crayfish and Shrimp. Nat. Prod. Res. 2015, 29, 1477–1480. [Google Scholar] [CrossRef]
  27. Gachhi, D.B.; Hungund, B.S. Two-phase Extraction, Characterization, and Biological Evaluation of Chitin and Chitosan from Rhizopus oryzae. J. Appl. Pharm. Sci. 2018, 8, 116–122. [Google Scholar] [CrossRef]
  28. Narudin, N.A.H.; Rosman, N.A.; Shahrin, E.W.E.S.; Sofyan, N.; Mahadi, A.H.; Kusrini, E.; Hobley, J.; Usman, A. Extraction, Characterization, and Kinetics of N-deacetylation of Chitin Obtained from Mud Crab Shells. Polym. Polym. Compos. 2022, 30. [Google Scholar] [CrossRef]
  29. Nadarajah, K. Isolation and Characterization of Fungal Chitosan from Malaysian Isolates. J. Pure Appl. Micobiol. 2009, 3, 33–38. [Google Scholar]
  30. Kumari, S.; Rath, P.; Kumar, A.S.H.; Tiwari, T.N. Extraction and Characterization of Chitin and Chitosan from Fishery Waste by Chemical Method. Environ. Technol. Innov. 2015, 3, 77–85. [Google Scholar] [CrossRef]
  31. Al-Hassan, A.A. Utilization of Waste: Extraction and Characterization of Chitosan from Shrimp Byproducts. Civ. Environ. Res. 2016, 8, 117–123. [Google Scholar]
  32. Phase I/IIa Study on Chitin Microparticles in Subjects Suffering from Allergic Rhinitis. Available online: https://clinicaltrials.gov/ct2/show/NCT00443495 (accessed on 8 September 2023).
  33. Lee, C.G.; Da Silva, C.A.; Lee, J.-Y.; Hartl, D.; Elias, J.A. Chitin Regulation of Immune Responses: An Old Molecule with New Roles. Curr. Opin. Immunol. 2008, 20, 684–689. [Google Scholar] [CrossRef] [PubMed]
  34. Cuesta, A.; Esteban, M.A.; Meseguer, J. In Vitro Effect of Chitin Particles on the Innate Cellular Immune System of Gilthead Seabream (Sparus aurata L.). Fish Shellfish Immunol. 2003, 15, 1–11. [Google Scholar] [CrossRef] [PubMed]
  35. Kadry, M.O.; Abdel-Megeed, R.M.; El-Meliegy, E.; Abdel-Hamid, A.-H.Z. Crosstalk between GSK-3, c-Fos, NFκB and TNF-α Signaling Pathways Play an Ambitious Role in Chitosan Nanoparticles Cancer Therapy. Toxicol. Rep. 2018, 5, 723–727. [Google Scholar] [CrossRef] [PubMed]
  36. Liu, T.; Zhang, L.; Joo, D.; Sun, S.C. NF-κB Signaling in Inflammation. Signal Transduct. Target. Ther. 2017, 2, 17023. [Google Scholar] [CrossRef]
  37. Liu, G.; Chen, S.; Guan, G.; Tan, J.; Al-Dhabi, N.A.; Wang, H.; Duraipandiyan, V.; Fang, J. Chitosan Modulates Inflammatory Responses in Rats Infected with Enterotoxigenic Escherichia coli. Mediat. Inflamm. 2016, 2016, 7432845. [Google Scholar] [CrossRef]
  38. Choi, E.H.; Yang, H.P.; Chun, H.S. Chitooligosaccharide Ameliorates Diet-Induced Obesity in Mice and Affects Adipose Gene Expression Involved in Adipogenesis and Inflammation. Nutr. Res. 2012, 32, 218–228. [Google Scholar] [CrossRef]
  39. Wang, Z.F.; Wang, M.Y.; Yu, D.H.; Zhao, Y.; Xu, H.M.; Zhong, S.; Sun, W.Y.; He, Y.F.; Niu, J.Q.; Gao, P.J.; et al. Therapeutic Effect of Chitosan on CCl4-induced Hepatic Fibrosis in Rats. Mol. Med. Rep. 2018, 18, 3211–3218. [Google Scholar] [CrossRef]
  40. Huang, W.; Zhao, D.; Guo, N.; Xue, C.; Mao, X. Green and Facile Production of Chitin from Crustacean Shells Using a Natural Deep Eutectic Solvent. Agric. Environ. Chem. 2018, 66, 11897–11901. [Google Scholar] [CrossRef]
  41. Komi, D.E.A.; Sharma, L.; Dela Cruz, C.S. Chitin and Its Effects on Inflammatory and Immune Responses. Clin. Rev. Allergy Immunol. 2018, 54, 213–223. [Google Scholar] [CrossRef]
  42. The Indonesian Standardization Agency (1992) Methods for Analyzing Food and Beverages (SNI 01-2891-1992). Available online: https://legalcentric.com/content/view/151630 (accessed on 8 September 2023).
  43. Wang, H.; Roman, M. Effects of Chitosan Molecular Weight and Degree of Deacetylation on Chitosan−Cellulose Nanocrystal Complexes and Their Formation. Molecules 2023, 28, 1361. [Google Scholar] [CrossRef]
  44. Percie du Sert, N.; Hurst, V.; Ahluwalia, A.; Alam, S.; Avey, M.T.; Baker, M.; Browne, W.J.; Clark, A.; Cuthill, I.C.; Dirnagl, U.; et al. The ARRIVE guidelines 2.0: Updated guidelines for reporting animal research. PLoS Biol. 2020, 177, 3617–3624. [Google Scholar] [CrossRef]
  45. Almasaudi, S.B.; El-Shitany, N.A.; Abbas, A.T.; Abdel-Dayem, U.A.; Ali, S.S.; Al Jaouni, S.K.; Harakeh, S. Antioxidant, Anti-inflammatory, and Antiulcer Potential of Manuka Honey against Gastric Ulcer in Rats. Oxid. Med. Cell. Longev. 2016, 2016, 3643824. [Google Scholar] [CrossRef] [PubMed]
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Figure 1. The after-boiled shells of blue swimming crabs (Portunus pelagicus Linn.) were collected in Gunung Jati Cirebon, West Java, Indonesia.
Figure 1. The after-boiled shells of blue swimming crabs (Portunus pelagicus Linn.) were collected in Gunung Jati Cirebon, West Java, Indonesia.
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Figure 2. The % transmittance FT-IR spectrum of chitin extracted from the shells of blue swimming crabs (P. pelagicus Linn.) recorded at 4000 to 500 cm−1 revealing the OH stretch band at 3434.64 cm−1 superimposed on NH stretching band (occurs as shoulder bands at 2937.72 cm−1); the amide C=O band at 1620.41 cm−1; the amide –CN band at 1425.51 cm−1; the alkyl C-H band at 1388.06 cm−1; the −CN of amino groups between 1155.90 and 1201.06 cm−1; and the polysaccharide bands are detected between 566.58 and 1031.90 cm−1.
Figure 2. The % transmittance FT-IR spectrum of chitin extracted from the shells of blue swimming crabs (P. pelagicus Linn.) recorded at 4000 to 500 cm−1 revealing the OH stretch band at 3434.64 cm−1 superimposed on NH stretching band (occurs as shoulder bands at 2937.72 cm−1); the amide C=O band at 1620.41 cm−1; the amide –CN band at 1425.51 cm−1; the alkyl C-H band at 1388.06 cm−1; the −CN of amino groups between 1155.90 and 1201.06 cm−1; and the polysaccharide bands are detected between 566.58 and 1031.90 cm−1.
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Marinedrugs 21 00488 g003
Figure 3. Hematoxylin-eosin staining of rat stomach organs (B = bleeding, DE = desquamated epithelium, FD = fat degeneration, HD = hydropic degeneration, ICI = inflammatory cell infiltration: (1) positive control group; (2) negative control group; (3) normal control group; (4–6) chitin extracts (150 mg/kg BW, 300 mg/kg BW, and 600 mg/kg BW); (7–9) commercial chitins (150 mg/kg BW, 300 mg/kg BW, and 600 mg/kg BW); (10, 11) crude shell powder (500 mg/kg BW and 1000 mg/kg BW). All microscopic images used an ocular lens magnification of 12× and an object lens of 10×. All experiments were replicated 3×.
Figure 3. Hematoxylin-eosin staining of rat stomach organs (B = bleeding, DE = desquamated epithelium, FD = fat degeneration, HD = hydropic degeneration, ICI = inflammatory cell infiltration: (1) positive control group; (2) negative control group; (3) normal control group; (4–6) chitin extracts (150 mg/kg BW, 300 mg/kg BW, and 600 mg/kg BW); (7–9) commercial chitins (150 mg/kg BW, 300 mg/kg BW, and 600 mg/kg BW); (10, 11) crude shell powder (500 mg/kg BW and 1000 mg/kg BW). All microscopic images used an ocular lens magnification of 12× and an object lens of 10×. All experiments were replicated 3×.
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Marinedrugs 21 00488 g004
Figure 4. Effect of different doses of chitins in the form of extracts, commercials, and shell powders on the hemorrhagic severity of the gastric mucosa in ethanol-induced gastric ulceration rats: (1) positive control group: intact gastric mucosa tissues; (2) negative control group: severe hemorrhage; (3) normal control group; (4–6) chitin extracts (150 mg/kg BW, 300 mg/kg BW, and 600 mg/kg BW): mild hemorrhagic on the gastric mucosa; (7–9) commercial chitins (150 mg/kg BW, 300 mg/kg BW, and 600 mg/kg BW): mild hemorrhagic on the gastric mucosa; (10, 11) shell powders (500 mg/kg BW and 1000 mg/kg BW): mild hemorrhagic on the gastric mucosa. All experiments were replicated 3×.
Figure 4. Effect of different doses of chitins in the form of extracts, commercials, and shell powders on the hemorrhagic severity of the gastric mucosa in ethanol-induced gastric ulceration rats: (1) positive control group: intact gastric mucosa tissues; (2) negative control group: severe hemorrhage; (3) normal control group; (4–6) chitin extracts (150 mg/kg BW, 300 mg/kg BW, and 600 mg/kg BW): mild hemorrhagic on the gastric mucosa; (7–9) commercial chitins (150 mg/kg BW, 300 mg/kg BW, and 600 mg/kg BW): mild hemorrhagic on the gastric mucosa; (10, 11) shell powders (500 mg/kg BW and 1000 mg/kg BW): mild hemorrhagic on the gastric mucosa. All experiments were replicated 3×.
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Figure 5. (a) The bands of NF-kappaB p65 (65 kDa) and β-actin (42 kDa) in the stomach of the Wistar rats by Western blot analysis; (b) The relative expression of NF-kappaB p65 normalized to β-actin in all rat models: (1) positive control group; (2) negative control group; (3) normal control group; (4–6) chitin extracts (150 mg/kg BW, 300 mg/kg BW, and 600 mg/kg BW); (7–9) commercial chitins (150 mg/kg BW, 300 mg/kg BW, and 600 mg/kg BW); (10, 11) shell powders (500 mg/kg BW and 1000 mg/kg BW). * p < 0.05 means significantly different compared with the negative control group. All experiments were replicated 3×.
Figure 5. (a) The bands of NF-kappaB p65 (65 kDa) and β-actin (42 kDa) in the stomach of the Wistar rats by Western blot analysis; (b) The relative expression of NF-kappaB p65 normalized to β-actin in all rat models: (1) positive control group; (2) negative control group; (3) normal control group; (4–6) chitin extracts (150 mg/kg BW, 300 mg/kg BW, and 600 mg/kg BW); (7–9) commercial chitins (150 mg/kg BW, 300 mg/kg BW, and 600 mg/kg BW); (10, 11) shell powders (500 mg/kg BW and 1000 mg/kg BW). * p < 0.05 means significantly different compared with the negative control group. All experiments were replicated 3×.
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Figure 6. The rat’s stomach after ethanol-induced ulcerative at the time of (A) 30 min; (B) 1 h; (C) 1.5 h; (D) 2 h.
Figure 6. The rat’s stomach after ethanol-induced ulcerative at the time of (A) 30 min; (B) 1 h; (C) 1.5 h; (D) 2 h.
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Table 1. Effect of different doses of chitin extract, commercial chitin, and crude shell powder on the % relative stomach weight and % ulcer index in ethanol-induced gastric ulceration rats.
Table 1. Effect of different doses of chitin extract, commercial chitin, and crude shell powder on the % relative stomach weight and % ulcer index in ethanol-induced gastric ulceration rats.
Rat GroupStomach Index (%) ± SDUlcer Index (%)
Positive control group 0.62 ± 0.030.17 ± 0.11 *
Negative control group0.63 ± 0.0914.55 ± 2.62 #
Normal control group0.57 ± 0.040.06 ± 0.06 *
Chitin extract 150 mg/kg BW0.54 ± 0.044.79 ± 4.37 *
Chitin extract 300 mg/kg BW0.51 ± 0.021.08 ± 0.77 *
Chitin extract 600 mg/kg BW0.49 ± 0.031.60 ± 0.44 *
Commercial chitin 150 mg/kg BW0.72 ± 0.142.94 ± 1.74 *
Commercial chitin 300 mg/kg BW0.62 ± 0.161.32 ± 0.44 *
Commercial chitin 600 mg/kg BW0.59 ± 0.054.80 ± 0.66 *
Crude shell powder 500 mg/kg BW0.59 ± 0.031.50 ± 1.17 *
Crude shell powder 1000 mg/kg BW0.60 ± 0.071.42 ± 0.77 *
Statistical analysis was done using IBM SPSS Statistics version 24.0 for Windows. All experiments were replicated 3×. Data are presented as mean ± SD. * Indicates a significant difference (p < 0.05) compared to the negative control group. # Indicates a significant difference (p < 0.05) compared to the normal control group.
Table 2. Effect of different doses of chitin extract, commercial chitin, and crude shell powder on the number of necrotic cells, normal cells, and % fat degeneration in ethanol-induced gastric ulceration rats.
Table 2. Effect of different doses of chitin extract, commercial chitin, and crude shell powder on the number of necrotic cells, normal cells, and % fat degeneration in ethanol-induced gastric ulceration rats.
Rat GroupNecrotic CellsNormal CellsFat Degeneration
Positive control group 5788322
Negative control group8883648
Normal control group4391120
Chitin extract 150 mg/kg BW4788820
Chitin extract 300 mg/kg BW6786426
Chitin extract 600 mg/kg BW6386124
Commercial chitin 150 mg/kg BW6287923
Commercial chitin 300 mg/kg BW5588021
Commercial chitin 600 mg/kg BW5888219
Crude shell powder 500 mg/kg BW6785125
Crude shell powder 1000 mg/kg BW7784823
No statistical analysis was done. Counting and observation were done 1× for each group.
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MDPI and ACS Style

Amelia, R.; Sumiwi, S.A.; Saptarini, N.M.; Levita, J. Chitin Extracted from the Shell of Blue Swimming Crabs (Portunus pelagicus Linn.) Inhibits NF-kappaB p65 in Ethanol-Induced Gastric Ulcerative Wistar Rats. Mar. Drugs 2023, 21, 488. https://doi.org/10.3390/md21090488

AMA Style

Amelia R, Sumiwi SA, Saptarini NM, Levita J. Chitin Extracted from the Shell of Blue Swimming Crabs (Portunus pelagicus Linn.) Inhibits NF-kappaB p65 in Ethanol-Induced Gastric Ulcerative Wistar Rats. Marine Drugs. 2023; 21(9):488. https://doi.org/10.3390/md21090488

Chicago/Turabian Style

Amelia, Renny, Sri Adi Sumiwi, Nyi Mekar Saptarini, and Jutti Levita. 2023. "Chitin Extracted from the Shell of Blue Swimming Crabs (Portunus pelagicus Linn.) Inhibits NF-kappaB p65 in Ethanol-Induced Gastric Ulcerative Wistar Rats" Marine Drugs 21, no. 9: 488. https://doi.org/10.3390/md21090488

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