Abstract
Antarctic ice microalgae (Chlamydomonas sp.) are a polysaccharide-rich natural marine resource. In this study, we evaluated the impact of Antarctic ice microalgae polysaccharides (AIMP) on D-galactose-induced oxidation in mice. We conducted biological and biochemical tests on tissue and serum samples from mice treated with AIMP. We found that AIMP administration was associated with improved thymus, brain, heart, liver, spleen, and kidney index values. We also found that AIMP treatment inhibited the reduced aspartate aminotransferase, alanine aminotransferase, alkaline phosphatase, superoxide dismutase, glutathione peroxidase, and glutathione levels as well as the increased serum, splenic, and hepatic nitric oxide and malondialdehyde levels arising from oxidation in these animals. Pathological examination revealed that AIMP also inhibited D-galactose-induced oxidative damage to the spleen, liver, and skin of these animals. AIMP was additionally found to promote the upregulation of neuronal nitric oxide synthase, endothelial nitric oxide synthase, cuprozinc-superoxide dismutase, manganese superoxide dismutase, catalase, heme oxygenase-1, nuclear factor erythroid 2-related factor 2, γ-glutamylcysteine synthetase, and NAD(P)H dehydrogenase [quinone] 1 as well as the downregulation of inducible nitric oxide synthase in these animals. High-performance liquid chromatography analysis revealed AIMP to be composed of five monosaccharides (mannitol, ribose, anhydrous glucose, xylose, and fucose). Together, these results suggest that AIMP can effectively inhibit oxidative damage more readily than vitamin C in mice with D-galactose-induced oxidative damage, which underscores the value of developing AIMP derivatives for food purposes.
Introduction
Antarctic ice microalgae (Chlamydomonas sp.) are found in both fixed and floating ice in the Antarctic sea. Due to the extreme and prolonged cold in this region, Antarctic ice microalgae have significant physiological and morphological differences when compared to other forms of algae. Antarctic ice microalgae are collagen-rich, yellow-to-brown organisms that contain high levels of calcium, iron, iodine, phosphorus, and cellulose, and their mineral element content levels are higher than those in Chlamydomonas monadina (). Studies of these microalgae began in the 1960s (), and recent work has resulted in more deeply characterization of the biochemical and physiological properties of these organisms. In traditional Chinese medicine, Antarctic ice microalgae are considered to protect the skin and soften the blood vessels (). However, up to now, few studies have evaluated the biological activity of Antarctic ice microalgae. At present, only a single study has shown that there are antioxidant enzymes in Antarctic ice algae, which may have antioxidant effects (). However, other microalgae have been shown to have antioxidant effects. 2, 2 diphenyl-1-picrylhydrazyl (DPPH) test and 2,2′-azino-bis (ethylbenzthiazoline-6-sulfonic acid (ABTS.+) experiments showed that the extracts of some microalgae had good ability of scavenging free radicals in vitro, and they were antioxidants (). In addition, in vitro study also confirmed that a variety of microalgae were non-toxic and had inhibitory effect on DNA oxidative damage and cell oxidative damage caused by H2O2 (). As one of the most widely used microalgae, Arthrospira platensis has been confirmed by animal experiments and clinical experiments to have antioxidant effect and regulate a variety of diseases including hypercholesterolemia, hypertriglyceridemia, cardiovascular disease and inflammatory disease through its antioxidant capacity (). At the same time, a variety of microalgae also have good antioxidant effect, such as Tetraselmis suecica, Botryococcus braunii, Neochloris oleoabundans and so on, they all contain polysaccharide substances and have the potential as a source of natural antioxidants (). Meanwhile, polysaccharides as important bioactive substances have been confirmed to have antioxidant and anti-inflammatory effects through in vitro cell studies and in vivo animal experiments (–). The active ingredients in some seaweeds can be used to develop antioxidant foods and drugs. However, in terms of traditional health care products, Antarctic ice algae still lack scientific evidence proving their biological activity, which hinders their development and use. This study is the first to analyze the antioxidant effectiveness of Antarctic ice microalgae as medicinal and health care products.
Normal homeostasis depends on balanced oxidative and antioxidative activity in vivo. A small amount of reactive oxygen species (ROS) can clear viruses from the body, but a large amount of ROS in the body will cause oxidative damage (, ). The intake of nutrients can effectively reduce lipid peroxidation and oxidative stress ().
D-galactose can establish an effective oxidative damage state in animals (). In this study, we also used D-galactose to establish an oxidative damage model in mice to test the antioxidant effect of Antarctic ice algae polysaccharide (AIMP) and its regulatory effect on HO-1, the key expression of oxidation. The impacts of AIMP on serum and tissue changes in these animals were examined. By assessing AIMP-induced changes in the expression levels of oxidation-related genes, we evaluated the mechanisms whereby AIMP inhibits oxidative stress, thus providing a theoretical basis for future studies regarding the use and pharmaceutical development of AIMP.
Materials and Methods
AIMP Extraction and Purification
Antarctic ice algae are mainly found off the southern coast of Chile, and the samples used in this study were from this area. Initially, a sample (500 g) of Antarctic ice microalgae (Qingdao Shenshoutang Seafood Co., Ltd., Qingdao, Shandong, China) was ultrasonically extracted in 2.5 L of ddH2O for 40 min at 90°C to facilitate polysaccharide extraction. The resultant solution was filtered through sterile gauze. The filtered residue was collected, resuspended in water, and ultrasonically extracted (CYS-Y21S Ultrasonic Extractor, Hangzhou Supersonic Electromechanical Technology Co., Ltd., Hangzhou, China) at 600W for 20 min. These steps were repeated thrice. The three extract preparations were combined, freeze-dried, and resuspended in a small volume of hot water. Next, ethanol was added to a final concentration of 80% EtOH. The samples were then freeze-dried for 8 h. The samples were then again resuspended in water and 80% EtOH and allowed to stay overnight at 4°C. The samples were then freeze-dried a final time to isolate the crude polysaccharides. The Sevag method was then used four times to isolate the crude polysaccharides dissolved in hot water (). These four aqueous samples were subsequently combined. A small quantity of activated carbon was added to this solution, which was then allowed to stay for 10 min prior to filtration. EtOH was added to the filtrate to a final concentration of 80% EtOH, and the samples were again allowed to stay at 4°C overnight. The final refined AIMP preparation was obtained by fully freeze-drying the samples and then transferring them to a vacuum drying oven for 4 h.
Animal Model
We obtained fifty 6-week-old ICR mice (25 males, 25 females; SPF-grade, Chongqing Medical University, Chongqing, China). The animals were allowed to acclimatize for 1 week prior to being assigned at random to one of five different treatment groups (n = 10/group; five males, five females/group): a control group, a model group (oxidative damage control group), a low-dose AIMP group (AIMP-L), a high-dose AIMP group (AIMP-H), and a vitamin C treatment group (Vit C). The mice in the control and model groups were fed standard food and water for 6 weeks. The mice in the AIMP-L and AIMP-H groups were treated with 50 mg/kg or 100 mg/kg of AIMP, respectively, by gavage each day for 6 weeks. During this same 6-week period, the mice in the Vit C group were treated with 100 mg/kg of Vit C by gavage each day. In these 6 weeks, the mice in each group except for the control group were also intraperitoneally injected once per day with 120 mg/kg of D-galactose (Figure 1). After the treatment period ended, the mice were fasted for 24 h before being euthanized (). Blood samples were collected from the hearts of the mice, and liver and splenic tissue samples were collected for downstream analyses. Thymus, brain, heart, liver, spleen, and kidney organ index values were determined as follows:
Figure 1
Assessment of ALT, AST, AKP, NO, GSH, and MDA Levels and SOD and GSH-Px Activity
Blood samples from all mice were spun for 10 min at 4,000 rpm. The serum was then isolated and used to assess the levels of alanine aminotransferase (ALT), aspartate aminotransferase (AST), alkaline phosphatase (AKP), nitric oxide (NO), glutathione (GSH) and malondialdehyde (MDA) and the activity of superoxide dismutase (SOD) and glutathione peroxidase (GSH-Px) using appropriate test kits (Nanjing Jiancheng Bioengineering Institute, Nanjing, Jiangsu, China). The 10 μL serum of each mouse were determined these indexes used the kits and finally, the indexes were calculated by the absorbance. For the hematic samples, 10% homogenates were prepared prior to spinning for 10 min at 4,000 rpm. The supernatants were then collected, and the levels of NO, GSH and MDA and the activity of SOD and GSH-Px were assessed using appropriate test kits (Nanjing Jiancheng Bioengineering Institute, Nanjing, Jiangsu, China).
Assessment of Hepatic and Splenic Morphology
Murine hepatic and splenic tissue samples (~0.5 cm3) were isolated, fixed for 48 h with 10% formalin, embedded in paraffin, sectioned, and stained with hematoxylin and eosin. A light microscope (BX43, Olympus, Tokyo, Japan) was then used to evaluate tissue morphology.
Quantitative PCR
RNAzol (Invitrogen, Carlsbad, CA, USA) was used to extract the total RNA from the hepatic and splenic tissue homogenates. The RNA was diluted to a concentration of 1 μg/μL with enzyme-free water, and then 1 μL of the diluted RNA and 9 μL of oligo (dT) primer were put into the polymerase chain reaction (PCR) apparatus at 65°C for 5 min to complete a thermal cycle. Next, 4 μL of 5× reaction buffer, 1 μL of RiboLock RNase inhibitor, 2 μL of 100 mM dNTP mix, and 1 μL of RevertAid Reverse Transcriptase were added and then mixed. The cDNA template was generated via PCR at 42°C for 60 min and 70°C for 5 min. Next, 2 μL of this cDNA template per sample was combined with 10 μL of SYBR Green PCR Master Mix and 1 μL of forward and reverse primers (Thermo Fisher Scientific, Waltham, MA, USA; Table 1). The following thermocycler settings were used: 95°C for 60 s, 40 cycles at 95°C for 15 s, 55°C for 30 s, and 72°C for 33 s. GAPDH was used to normalize gene expression, with the 2−ΔΔCt method being used to assess relative gene expression (StepOnePlus Real-Time PCR System, Thermo Fisher Scientific, Waltham, MA, USA) ().
Table 1
| Gene name | Sequence |
|---|---|
| nNOS | Forward: 5′-ACGGCAAACTGCACAAAGC-3′ |
| Reverse: 5′-CGTTCTCTGAATACGGGTTGTTG-3′ | |
| eNOS | Forward: 5′-TCAGCCATCACAGTGTTCCC-3′ |
| Reverse: 5′-ATAGCCCGCATAGCGTATCAG-3′ | |
| iNOS | Forward: 5′-GTTCTCAGCCCAACAATACAAGA-3′ |
| Reverse: 5′-GTGGACGGGTCGATGTCAC-3′ | |
| Cu/Zn-SOD | Forward: 5′-AACCAGTTGTGTTGTCAGGAC-3′ |
| Reverse: 5′-CCACCATGTTTCTTAGAGTGAGG-3′ | |
| Mn-SOD | Forward: 5′-CAGACCTGCCTTACGACTATGG-3′ |
| Reverse: 5′-CTCGGTGGCGTTGAGATTGTT-3′ | |
| CAT | Forward: 5′- GGAGGCGGGAACCCAATAG−3′ |
| Reverse: 5′- GTGTGCCATCTCGTCAGTGAA-3′ | |
| HO-1 | Forward: 5′-ACAGATGGCGTCACTTCG-3′ |
| Reverse: 5′-TGAGGACCCACTGGAGGA-3′ | |
| Nrf2 | Forward: 5′-CAGTGCTCCTATGCGTGAA-3′ |
| Reverse: 5′-GCGGCTTGAATGTTTGTC-3′ | |
| γ-GCS | Forward: 5′-GCACATCTACCACGCAGTCA-3′ |
| Reverse: 5′-CAGAGTCTCAAGAACATCGCC-3′ | |
| NQO1 | Forward: 5′-CTTTAGGGTCGTCTTGGC-3′ |
| Reverse: 5′-CAATCAGGGCTCTTCTCG-3′ | |
| GAPDH | Forward: 5′-AGGTCGGTGTGAACGGATTTG-3′ |
| Reverse: 5′-GGGGTCGTTGATGGCAACA-3′ |
Primer sequences used in this study.
Western Blotting
According to the experimental method of Liu et al. (), 1 mL of radioimmunoprecipitation assay buffer containing 10 μL of phenylmethylsulfonyl fluoride (Thermo Fisher Scientific, MA, USA) was used to lyse the hepatic and splenic tissue sections for 5 min. They were then spun for 15 min at 12,000 rpm and 4°C. The protein levels in these samples were assessed via bicinchoninic acid assay (Thermo Fisher Scientific), after which they were diluted to 50 μg/mL. The samples were then mixed with sample buffer (4:1) and denatured for 5 min by heating to 100°C. They were then chilled on ice for 5 min. The samples were then separated via sodium dodecyl sulfate-polyacrylamide gel electrophoresis using previously prepared gels, with a pre-stained protein ladder used for reference. The proteins were next transferred to polyvinylidene fluoride membranes that were then blocked for 1 h using 5% non-fat milk in TBST. The blots were then incubated with 1 μg/mL primary antibodies of nNOS, eNOS, iNOS, Cu/Zn-SOD, Mn-SOD, CAT, HO-1, Nrf2 and NQO1 at 25°C for 2 h. They were then washed five times with TBST and then incubated with 0.4 μg/mL Goat anti-Mouse IgG secondary antibodies (Thermo Fisher Scientific) at 25°C for 1 h. SuperSignal West Pico PLUS reagent was then used to detect the protein bands with an imaging system (Tanon 5200, Shanghai Tanon Technology Co., Ltd., Shanghai, China).
Derivative Product Preparation
Initially, standard mixtures of monosaccharides were prepared by mixing 100 μL of 0.5 mol/L PMP-methanol and 100 μL of 0.3 mol/L NaOH with 100 μL of the mixed standard solution of each monosaccharide. This solution was mixed for 1 min, then the derivatization reaction was conducted for 40 min at 60°C in a water bath. The samples were then cooled to room temperature, and 100 μL of 0.3 mol/L sample was used. Next, HCl was neutralized in this solution, and 2 mL of chloroform was added. The supernatants were collected and extracted thrice via vortexing for 1 min. An AIMP hydrolysate sample was also derived via this same approach.
High-Performance Liquid Chromatography
The AIMP was initially dissolved to 10 mg/mL using dimethyl sulfoxide, then it was diluted to 2 mg/mL using 50% methanol. The AIMP samples and standard solutions were then passed through a 0.22-μm membrane, and 10 μL of each solution was subjected to high-performance liquid chromatography analysis. The mobile phase for this analysis was composed of an ammonium acetate buffer solution (A) (0.05 mol/L, pH=5.5) and acetonitrile (B). A 10-μL injection volume was used, and the column was maintained at 30°C with a flow rate of 1.0 mL/min and a wavelength of 250 nm. The gradient settings were: 0 to 30 min, 1-18% B; 30 to 50 min, 18-25% B; and 50 to 60 min, 25-30% B (UltiMate 3000, Thermo Fisher Scientific, Inc., Waltham, MA, USA).
Statistical Analysis
All samples were analyzed in triplicate. SAS 9.1 software (SAS Institute Inc., Cary, NC, USA) was used for all statistical testing. Data were compared via one-way analysis of variance, with p < 0.05 as the significance threshold.
Results
Component Analysis of AIMP
The high-performance liquid chromatography analysis results revealed AIMP to be primarily composed of mannitol (236.12 ± 1.05 mg), ribose (15.02 ± 0.56 mg), anhydrous glucose (14.19 ± 0.31 mg), xylose (17.82 ± 0.36 mg), and fucose (462.33 ± 1.11 mg, Figure 2), with the fucose content being the highest.
Figure 2
Toxicity, Weight and Organ Index
The model group mice exhibited lower thymic, hepatic, splenic, renal, and brain index values than did the mice in the other groups, while these values were maximal in the control group mice (Table 2). AIMP and Vit C treatments were associated with significant improvements in these organ index values in the D-galactose-treated mice (p < 0.05), with AIMP-induced improvements being significantly better than Vit C-induced improvements. Together, these findings suggest that AIMP treatment is sufficient to inhibit oxidative damage-induced declines in organ index values in D-galactose-treated mice.
Table 2
| Group | Control | Model | Vit C | AIMP-L | AIMP-H | |
|---|---|---|---|---|---|---|
| Body | Weight (g) | 36.48 ± 3.27a | 34.78 ± 3.69a | 35.48 ± 4.08a | 35.22 ± 3.68a | 36.29 ± 3.83a |
| Thymus | Weight (mg) | 74.05 ± 4.32a | 31.65 ± 2.17e | 53.93 ± 3.44c | 42.81 ± 2.98d | 62.42 ± 3.79b |
| Index | 2.03 ± 0.20a | 0.91 ± 0.18e | 1.52 ± 0.11c | 1.22 ± 0.08d | 1.72 ± 0.12b | |
| Brain | Weight (mg) | 767.17 ± 12.35a | 374.93 ± 8.20e | 583.29 ± 6.60c | 418.77 ± 8.23d | 657.21 ± 10.36b |
| Index | 21.03 ± 0.42a | 10.78 ± 0.23e | 16.44 ± 0.34c | 11.89 ± 0.32d | 18.11 ± 0.20b | |
| Cardiac | Weight (mg) | 191.52 ± 6.79a | 140.86 ± 4.97e | 162.14 ± 4.06c | 148.63 ± 6.22d | 178.91 ± 6.11b |
| Index | 5.25 ± 0.05a | 4.05 ± 0.05e | 4.57 ± 0.06c | 4.22 ± 0.03d | 4.93 ± 0.05b | |
| Liver | Weight (mg) | 1508.45 ± 35.67a | 942.89 ± 12.36e | 1172.61 ± 25.32c | 1100.63 ± 30.25d | 1360.88 ± 32.09b |
| Index | 41.35 ± 0.31a | 27.11 ± 0.22e | 33.05 ± 0.26c | 31.25 ± 0.24d | 37.50 ± 0.29b | |
| Spleen | Weight (mg) | 161.61 ± 6.12a | 70.60 ± 5.31e | 123.12 ± 7.10c | 99.67 ± 7.85d | 142.62 ± 4.33b |
| Index | 4.43 ± 0.24a | 2.03 ± 0.20e | 3.47 ± 0.25c | 2.83 ± 0.19d | 3.93 ± 0.21b | |
| Kidney | Weight (mg) | 542.82 ± 5.98a | 279.98 ± 9.33e | 399.50 ± 6.92c | 348.33 ± 6.32d | 472.13 ± 5.12b |
| Index | 14.88 ± 0.11a | 8.05 ± 0.09e | 11.26 ± 0.16c | 9.89 ± 0.16d | 13.01 ± 0.14b | |
Organ index values in treated mice (N = 10).
Data are means ± standard deviations (N = 10/group).
Different superscript letters within a row correspond to significant differences (p < 0.05; Duncan's multiple range test). Vc: mice treated with 100 mg/kg vitamin C; AIMP-L: mice treated with 50 mg/kg AIMP; AIMP-H: treatment with 100 mg/kg AIMP.
Histology Analysis
The control group mice exhibited standard hepatic histology, with hepatocytes being radially arranged in an ordered fashion around the central vein and with no evidence of inflammatory cell infiltration (Figure 3). In contrast, the model group mice exhibited erratic and disordered hepatocyte arrangement, with irregular cell morphological findings, such as damaged nuclei, swelling, and the breakdown of the barriers between the cells. Substantial inflammatory infiltration was also observed in the liver samples of the D-galactose-treated mice. Treatment with AIMP was associated with the reversal of the D-galactose-induced damage, with less cellular disorder being evident in the hepatic sections from the mice administered this polysaccharide mixture. AIMP-H treatment resulted in maximal preservation of hepatic cell integrity, with the samples from the AIMP-H-treated mice being most similar to those from the control group mice.
Figure 3
The control group mice also exhibited normal splenic architecture, as evidenced by clearly ordered cells and regular tissue structure (Figure 4). In contrast, this ordered structure was absent in the D-galactose-treated mice in the model group. The model mice exhibited irregular morphological findings, expansion of the red pulp medullary sinuses, reduced numbers of white pulp lymphocytes, and sparser cell arrangement. AIMP treatment was associated with the reversal of the D-galactose-induced changes in splenic morphology. Together, these results suggest that AIMP treatment is sufficient to inhibit D-galactose-induced oxidative tissue damage in mice, and that this polysaccharide mixture is more beneficial than Vit C, at least in this experimental context.
Figure 4
Assessment of Oxidative Stress Markers
Assessment of ALT, AST, and AKP Levels in the Serum of the Treated Mice
The control group mice showed the lowest ALT, AST, and AKP serum levels, while these indexes were highest in the model group mice (Table 3). The ALT, AST, and AKP levels of the AIMP-H mice were closest to those of the control group mice, and these levels in the AIMP-H mice were significantly lower than those in the Vit C, AIMP-L, and model group mice (p < 0.05).
Table 3
| Group | ALT (U/L) | AST (U/L) | AKP (U/L) |
|---|---|---|---|
| Control | 15.35 ± 1.20e | 11.05 ± 1.05e | 31.22 ± 3.12e |
| Model | 61.37 ± 2.12a | 57.66 ± 1.97a | 93.59 ± 5.28a |
| Vit C | 36.02 ± 1.78c | 29.60 ± 1.55c | 62.80 ± 4.41c |
| AIMP-L | 45.62 ± 2.01b | 42.56 ± 2.38b | 46.08 ± 3.92b |
| AIMP-H | 28.33 ± 1.62d | 20.36 ± 1.73d | 75.10 ± 3.36d |
Serum ALT, AST, and AKP levels in treated mice (N = 10).
Data are means ± standard deviations (N = 10/group).
Different superscript letters within a column correspond to significant differences (p < 0.05; Duncan's multiple range test). Vc: mice treated with 100 mg/kg vitamin C; AIMP-L: mice treated with 50 mg/kg AIMP; AIMP-H: treatment with 100 mg/kg AIMP.
Expression of nNOS, eNOS, and iNOS in Hepatic and Splenic Samples
We next evaluated the neuronal nitric oxide synthase (nNOS), endothelial nitric oxide synthase (eNOS), and inducible nitric oxide synthase (iNOS) expression levels in the hepatic and splenic samples of the mice (Figures 5, 6). We found that relative to the mice in the other groups, the mice in the control group exhibited significant increases in the mRNA levels of nNOS and eNOS in both the spleen and liver as well as significant increases in the protein levels of nNOS and eNOS in the liver (p < 0.05). The mRNA levels of iNOS in the spleen and liver and the protein levels of iNOS in the liver of the mice in the control group were significantly lower than those in the mice in any other group (p < 0.05). D-galactose treatment was associated with significant reductions in nNOS and eNOS expression levels and with significant increases in iNOS expression levels in both hepatic and splenic tissues. AIMP treatment was sufficient to significantly reverse the D-galactose-induced changes in all nitric oxide synthase (NOS) expression levels (p < 0.05), and it was more efficacious than an equivalent dose of Vit C treatment.
Figure 5
Figure 6
Expression of Cu/Zn-SOD, Mn-SOD, and CAT in Hepatic and Splenic Samples
We also evaluated the cuprozinc-superoxide dismutase (Cu/Zn-SOD), manganese superoxide dismutase (Mn-SOD), and catalase (CAT) mRNA levels in the hepatic and splenic samples and protein levels in the hepatic samples of the mice (Figures 7, 8). We found maximal expression levels of these markers in the control group mice. In contrast, the expression levels of these markers were downregulated in the model group mice. AIMP and Vit C treatments were associated with significant increases in hepatic and splenic CAT, Cu/Zn-SOD, and Mn-SOD expression levels in the D-galactose-treated mice (p < 0.05), with the levels in the AIMP-H-treated mice being closest to those in the control group mice.
Figure 7
Figure 8
Assessment of Hepatic and Splenic HO-1, Nrf2, γ-GCS, and NQO1 in the Treated Mice
We also evaluated the HO-1, nuclear factor erythroid 2-related factor 2 (Nrf2), γ-glutamylcysteine synthetase (γ-GCS), and NAD(P)H dehydrogenase [quinone] 1 (NQO1) mRNA levels in the hepatic and splenic samples and protein levels in the hepatic samples of the mice (Figures 9, 10). We found that relative to the mice in the other groups, these genes were expressed at significantly elevated levels in the mice in the control group (p < 0.05). In contrast, the model group mice exhibited the lowest levels of splenic HO-1, Nrf2, γ-GCS, and NQO1 expression. The levels of these genes in both the hepatic and splenic samples rose significantly in response to AIMP-H treatment, with the beneficial effects of this polysaccharide solution being superior to those of the AIMP-L and Vit C preparations (p < 0.05).
Figure 9
Figure 10
Assessment of Antioxidant Enzymes
Relative to the mice in the other treatment groups, the mice in the model group exhibited significant reductions in SOD and GSH-Px activity in the spleen, liver, and serum (Table 4), while the NO and MDA levels in the mice in the model group were higher than those in the mice in the other groups. The mice in the control group had maximal SOD, GSH-Px, and glutathione activity and the lowest NO and MDA levels. AIMP treatment was associated with significant increases in SOD, GSH-PX, and glutathione activity and significant reductions in MDA and NO levels (p < 0.05). Indeed, AIMP treatment resulted in these values being relatively close to those in the control group mice, and AIMP treatment was significantly better than Vit C treatment in terms of the ability to remediate the D-galactose-induced changes in antioxidant activity (p < 0.05).
Table 4
| Group | NO (μmol/L) | SOD (U/mL) | GSH-Px (U/mL) | GSH (mg/L) | MDA (nmol/mL) |
|---|---|---|---|---|---|
| Normal | 12.51 ± 0.25e | 244.89 ± 11.29a | 225.62 ± 12.08a | 51.08 ± 3.68a | 3.12 ± 0.32e |
| Model | 56.51 ± 1.23a | 56.36 ± 5.98e | 70.19 ± 7.73e | 8.02 ± 0.79e | 35.67 ± 1.12a |
| Vit C | 32.45 ± 1.71c | 165.30 ± 12.65c | 139.87 ± 10.61c | 31.88 ± 2.03c | 9.97 ± 0.54c |
| AIMP-L | 40.89 ± 1.69b | 88.71 ± 10.25d | 92.79 ± 9.11d | 21.05 ± 1.88d | 18.96 ± 1.08b |
| AIMP-H | 18.46 ± 1.08d | 210.38 ± 11.20b | 188.10 ± 11.50b | 41.10 ± 2.29b | 5.67 ± 0.42d |
| Group | NO (μmol/g protein) | SOD (U/mgprot) | GSH-Px (U/mgprot) | GSH (mg/ gprot) | MDA (nmol/mgprot) |
| Normal | 2.16 ± 0.16e | 94.65 ± 5.26a | 181.09 ± 9.75a | 14.55 ± 0.74a | 1.18 ± 0.15e |
| Model | 11.05 ± 0.75a | 18.79 ± 2.61e | 46.85 ± 4.91e | 1.68 ± 0.36e | 10.36 ± 0.63a |
| Vit C | 4.98 ± 0.42c | 68.47 ± 3.82c | 118.63 ± 8.13c | 6.79 ± 0.49c | 4.33 ± 0.23c |
| AIMP-L | 8.32 ± 0.35b | 42.58 ± 3.08d | 88.75 ± 4.23d | 3.66 ± 0.27d | 6.91 ± 0.28b |
| AIMP-H | 3.44 ± 0.22d | 80.69 ± 2.91b | 159.81 ± 6.79b | 10.25 ± 0.62b | 2.01 ± 0.20d |
| Normal | 1.69 ± 0.16e | 89.12 ± 8.69a | 135.10 ± 11.68a | 9.62 ± 0.70a | 0.60 ± 0.11e |
| Model | 9.88 ± 0.60a | 15.97 ± 4.11e | 31.20 ± 3.66e | 1.56 ± 0.47e | 7.32 ± 0.45a |
| Vit C | 4.23 ± 0.36c | 56.51 ± 6.03c | 86.36 ± 7.25c | 5.33 ± 0.63c | 2.97 ± 0.22c |
| AIMP-L | 6.99 ± 0.41b | 29.65 ± 4.28d | 51.58 ± 5.44d | 3.82 ± 0.32d | 4.89 ± 0.36b |
| AIMP-H | 2.06 ± 0.22d | 70.36 ± 5.12b | 114.59 ± 9.71b | 7.03 ± 0.38b | 1.12 ± 0.16d |
The NO, SOD, GSH-Px, GSH, and MDA levels of serum, hepatic tissue and splenic tissue in treated mice (N = 10).
Data are means ± standard deviations (N = 10/group).
Different superscript letters within a column correspond to significant differences (p < 0.05; Duncan's multiple range test). Vc: mice treated with 100 mg/kg vitamin C; AIMP-L: mice treated with 50 mg/kg AIMP; AIMP-H: treatment with 100 mg/kg AIMP.
Discussion
Antarctic ice algae (Chlamydomonas sp.) have the characteristics of common algae, and they are rich in polysaccharides (). Seaweed cells contain certain polysaccharides that play important roles in controlling cell division, regulating cell growth, and maintaining the normal metabolism of living organisms (). A variety of seaweed polysaccharides have biological activities, including scavenging free radicals in vitro, protecting cells from oxidative damage, and inhibiting oxidative damage in animals (–). In this study, mannitol, ribose, anhydrous glucose, xylose, and fucose were found in AIMP for the first time. We also observed AIMP's effects on chemically induced oxidative damage in mice, and we analyzed the relationships between its components and its effects. Mannitol is readily absorbed by the human gastrointestinal tract. After intake, however, it is partially metabolized and excreted in the urine. It can be used to treat nephropathy and to alleviate intracranial and intraocular pressure (). Ribose is an RNA component that is essential for normal physiology, and as a reducing sugar, it also exhibits antioxidant properties (). Glucose is an essential energy source for cells and a metabolic intermediate (). Xylose is a monosaccharide with anti-fungal and anti-bacterial properties that aids in intestinal probiotic growth (). Fucose is another physiologically active monosaccharide that is associated with inhibiting cancer metastasis, promoting immune functionality, and treating infections of the respiratory tract (). The high fucose levels in AIMP are likely associated with the antioxidant effects of AIMP preparations, with the other four monosaccharides also contributing to this efficacy.
Organ weights and organ index values are commonly used to evaluate physiological changes in vivo in animal model systems, and they are thus optimal readouts for oxidative damage (). In particular, the effect of oxidative stress on the liver and spleen is particularly obvious, and also in the thymus and brain. The index of these organs can effectively test the degree of oxidative damage (–). In the present study, we found that D-galactose treatment in mice was sufficient to induce significant decreases in organ index values that were consistent with oxidative damage. Importantly, AIMP treatment was sufficient to prevent this oxidative damage, with AIMP-treated mice exhibiting organ index values similar to those of healthy mice.
Oxidative stress induced by ROS is the common pathophysiological basis of many liver diseases (). ALT, AST, and AKP are important indicators of liver function. The liver is the main organ that produces AKP. When the liver is damaged, hepatocytes overproduce AKP and flow back into the blood through lymphatic channels and hepatic sinuses (). ALT and AST are mainly distributed in hepatocytes. When hepatocytes are part of necrotic tissue, ALT and AST are released into the blood circulation, resulting in elevated serum enzyme levels, which are positively correlated with the degree of liver tissue damage (). We found that AIMP reduced serum AST, ALT, and AKP levels and thereby alleviated liver injury caused by oxidative stress.
The activation of NOS and the production of NO will trigger the production of O2 and OH, leading to cell damage. The interaction of no and promotes the formation of OH− and (). Overexpression of iNOS and NO production will damage stress resistance, thus promoting brain aging and aggravation of inflammation (, ). eNOS can inhibit oxidative stress-induced vascular aging and protect tissues (). In addition, nNOS can protect myocardium, smooth muscle and skeletal muscle from oxidative damage (, ). iNOS is a proinflammatory cytokine and exogenous antioxidant inhibitor (, ). Oxidative stress in the organism production of a large amount of ROS can promote the activation of iNOS, which can affect the expression levels of nNOS and eNOS in tissues, seaweed polysaccharides can also play a role in inhibiting oxidative stress by regulating these expression (–). Herein, we found that AIMP treatment was sufficient to modulate the levels of NO, nNOS, eNOS, and iNOS in D-galactose-treated mice, helping return these levels to those found in the normal healthy (control group) mice by mitigating D-galactose-induced oxidative damage.
SOD can prevent the accumulation of superoxide radicals, thus preventing oxidative damage (). Oxidative damage, in turn, resulted in reduced levels of two major types of SOD (Cu/Zn SOD and Mn SOD) in the affected tissues (, ). CAT mainly exists in cytoplasm and mitochondria and is an antioxidant enzyme (). Under normal conditions, excessive ROS produced by cells is rapidly neutralized by the activities of CAT, SOD, GSH-Px and other enzymes (). Glutathione is capable of serving as a scavenger for free radicals within cells, thus reducing ROS-associated lipid peroxidation (, ). MDA is a lipid peroxide produced in response to oxidative damage, with MDA levels thus offering insight into in vivo oxidation levels (). Herein, we found that AIMP treatment restored SOD, CAT, glutathione, MDA, and GSH-Px levels in the mice administered D-galactose to levels closer to those in the healthy mice. This result suggests that AIMP preparations can mitigate oxidative damage in vivo.
HO-1 is a stress protein that is important for heme metabolism, and it is associated with key anti-inflammatory and antioxidant activities. HO-1 exerts cardioprotective and neuroprotective effects owing to its antioxidant activity in the context of atherosclerosis, hypertension, Alzheimer's disease, and other neuronal diseases (). Nrf2 is a key modulator of vascular endothelial integrity, and its altered functionality in response to oxidative stress can promote HO-1 expression as well as CAT and SOD transcription, thus improving antioxidant activity (). Nrf2 also regulates γ-GCS, and large quantities of excess ROS lead to Nrf2 activation and high levels of γ-GCS expression, which in turn stimulate glutathione synthesis (). Under homeostatic conditions, Nrf2 is bound by Keap1, but in response to oxidative stress, these two proteins dissociate and Nrf2 enters the nucleus, where it can bind to ARE elements to drive the expression of the antioxidant enzyme NQO1. This Nrf2/NQO1 signaling pathway is a key means whereby certain bioactive compounds exert their antioxidant effects (). Herein, we found that AIMP treatment was associated with Nrf2 activity and enhanced HO-1, γ-GCS, and NQO1 levels, thereby protecting tissues from oxidative damage.
Antarctic ice algae are from the high latitudes and cold areas of Antarctica, and the algae that survive this harsh environment (low temperature, low light, and high ultraviolet radiation) contain more antioxidants than algae from areas with temperate temperatures. The protein, polysaccharide, and polyunsaturated fatty acid levels in Antarctic ice algae are higher than those in algae from areas with temperate temperatures (). Antarctic ice algae are rich in antioxidants, and the antioxidant effect may be better than that of algae from areas with temperate temperatures. The polysaccharides of Antarctic ice microalgae were analyzed in this study. The high-quality monosaccharide composition was an important reason for the algae's good antioxidant properties, which was also proved by the results of the animal experiments. In addition, Antarctic ice algae taste good in traditional foods. However, its components may be affected in transportation and processing, which may affect its functional function. Therefore, a more simple and effective extraction method needs to be studied. At the same time, the AIMP is mainly composed of five kinds of monosaccharides, but the more complex molecular structure and proportion need further component analysis.
Marine microalgae diatoms, chlorophytes, rhodophytes and dinoflagellates all contain polysaccharides, which are composed of galactose, mannose, xylose and rhamnose. Other marine microalgae, such as P. cruentum, P. purpureum, Rhodella reticulata and R. maculate, contain 3-O-methyl-xylose, 3-O-methyl-rhamnose and 4-O-methyl-galactose in addition to the above monosaccharides (, ). Marine microalgae polysaccharides can protect against oxidative stress by regulating Nrf2/HO-1 and apoptosis-related signaling pathways, so as to repair oxidative stress-induced damage (). This study showed that AIMP also had a certain role in the activation of the Nrf2/HO-1 pathway, suggesting that it may play a regulatory role and also have an antioxidant effect. At the same time, AIMP showed some similarities with other seaweed polysaccharides. The mechanism of AIMP was similar to that of other seaweed polysaccharides, but the differences between the mechanisms need further study.
Conclusions
The results of this study showed that AIMP prevented oxidative damage induced by D-galactose in mice. The serum, hepatic, and splenic findings in the AIMP-treated mice were closer to those in the normal mice (control group) than to those in the Vit C-treated mice. Our results highlight the importance of future studies of the in vivo bioactivity of AIMP preparations and derivatives thereof. We conducted a preliminary evaluation of the monosaccharides comprising AIMP, but future work is needed to clarify how these individual components contribute to the overall physicochemical properties of AIMP preparations. The activity of AIMP in human body must also be evaluated, because the utilization of this polysaccharide in human digestive system may be different from that in mice. This study was a preliminary investigation of the components and antioxidant capacity of AIMP. The mechanism of action of AIMP and its impact on the human body have not yet been fully elucidated. Additional preclinical and clinical studies of AIMP will be invaluable for our understanding of the potential pharmacological utility of this natural marine resource. In depth research is beneficial to the development of effective nutrients or drugs.
Statements
Data availability statement
The original contributions presented in the study are included in the article/supplementary material, further inquiries can be directed to the corresponding author/s.
Ethics statement
The protocol for these experiments was approved by the Ethics Committee of Chongqing Collaborative Innovation Center for Functional Food (201905030B), Chongqing, China. The experimental process was in accordance with 2010/63/EU directive.
Author contributions
RY and LD performed the majority of the experiments and wrote the manuscript. JM and CL contributed to the data analysis. XZ and FT designed and supervised the study, and checked the final manuscript. All authors contributed to the article and approved the submitted version.
Funding
This research was funded by Chongqing University Innovation Research Group Project (CXQTP20033), China.
Conflict of interest
The authors declare that the research was conducted in the absence of any commercial or financial relationships that could be construed as a potential conflict of interest.
References
1.
DemchenkoEMikhailyukTColemanAWPröscholdT. Generic and species concepts in Microglena (previously the Chlamydomonas monadina group) revised using an integrative approach. Eur J Phycol. (2012) 47:264–90. 10.1080/09670262.2012.678388
2.
NilewskiCCarreiraEM. Recent advances in the total synthesis of chlorosulfolipids. Eur J Organ Chem. (2012) 2012:1685–98. 10.1002/ejoc.201101525
3.
ShiCJKanGFMiaoJLLiGY. Progress of the adversity acclimation of Antarctic ice microalgae. Marine Sci. (2010) 34:100–3. Available online at: http://d.wanfangdata.com.cn/periodical/ChlQZXJpb2RpY2FsQ0hJTmV3UzIwMjEwMTI1Eg1oeWt4MjAxMDA0ME4Ggg3bHg5ZDZqbw%3D%3D
4.
WangQFHouYHMiaoJLLiGY. Effect of UV-B radiation on the growth and antioxidant enzymes of Antarctic sea ice microalgae Chlamydomonas sp. ICE-L. Acta Phy Plantarum. (2009) 31:1097–102. 10.1007/s11738-009-0271-x
5.
ShanabSMMMostafaSSMShalabyEAMahmoudGI. Aqueous extracts of microalgae exhibit antioxidant and anticancer activities. Asian Pac J Trop Biomed. (2012) 8:608–15. 10.1016/S2221-1691(12)60106-3
6.
GuedesACGiãoMSSeabraRFerreiraACSTamagniniPMoradas-FerreiraPet al. Evaluation of the antioxidant activity of cell extracts from microalgae. Mar Drugs. (2013) 11:1256–70. 10.3390/md11041256
7.
DengRChowTJ. Hypolipidemic, antioxidant, and antiinflammatory activities of microalgae Spirulina. Cardiovasc Ther. (2010) 28:33–45. 10.1111/j.1755-5922.2010.00200.x
8.
GoirisKMuylaertKFraeyeIFoubertIBrabanterJDCoomanLD. Antioxidant potential of microalgae in relation to their phenolic and carotenoid content. J Appl Phycol. (2012) 24:1477–86. 10.1007/s10811-012-9804-6
9.
AnanthiSRaghavendranHRBSunilAGGayathriVRamakrishnanGVasanthiHR. In vitro antioxidant and in vivo anti-inflammatory potential of crude polysaccharide from Turbinaria ornata (Marine Brown Alga). Food Chem Toxicol. (2010) 48:187–92. 10.1016/j.fct.2009.09.036
10.
DuZLiuHZhangZLiP. Antioxidant and anti-inflammatory activities of Radix Isatidis polysaccharide in murine alveolar macrophages. Int J Biol Macromol. (2013) 58:329–35. 10.1016/j.ijbiomac.2013.04.037
11.
HuangWMLiangYQTangLJDingYWangXH. Antioxidant and anti-inflammatory effects of Astragalus polysaccharide on EA.hy926 cells. Exp Ther Med. (2013) 6:199–203. 10.3892/etm.2013.1074
12.
AjithTA. Ameliorating reactive oxygen species-induced in vitro lipid peroxidation in brain, liver, mitochondria and DNA damage by Zingiber officinale Roscoe. Indian J Clin Biochem. (2010) 25:67–73. 10.1007/s12291-010-0014-1
13.
DubouchaudHWalterLRigouletMBatandierC. Mitochondrial NADH redox potential impacts the reactive oxygen species production of reverse Electron transfer through complex I. J Bioenerg Biomembr. (2018) 50:367–77. 10.1007/s10863-018-9767-7
14.
LiDZhangYLiuYSunRXiaM. Purified anthocyanin supplementation reduces dyslipidemia, enhances antioxidant capacity, and prevents insulin resistance in diabetic patients. J Nutr. (2015) 145:742–8. 10.3945/jn.114.205674
15.
LiLXuMShenBLiMGaoQWeiSG. Moderate exercise prevents neurodegeneration in D-galactose-induced aging mice. Neural Regen Res. (2016) 11:807–15. 10.4103/1673-5374.182709
16.
LongXYanQCaiLLiGLuoX. Box-Behnken design-based optimization for deproteinization of crude polysaccharides in Lycium barbarum berry residue using the Sevag method. Heliyon. (2020) 6:e03888. 10.1016/j.heliyon.2020.e03888
17.
QianYZhangJZhouXYiRMuJLongXet al. Lactobacillus plantarum CQPC11 isolated from Sichuan pickled cabbages antagonizes d-galactose-induced oxidation and aging in mice. Molecules. (2018) 23:3026. 10.3390/molecules23113026
18.
LiCTanFYangJYangYGouYLiSet al. Antioxidant effects of Apocynum venetum tea extracts on d-galactose-induced aging model in mice. Antioxidants. (2019) 8:381. 10.3390/antiox8090381
19.
LiuBZhangJSunPYiRHanXZhaoX. Raw Bowl tea (Tuocha) polyphenol prevention of nonalcoholic fatty liver disease by regulating intestinal function in mice. Biomolecules. (2019) 9:435. 10.3390/biom9090435
20.
PresaFBMarquesMLMVianaRLSNobreLTDBCostaLSRochaHAO. The protective role of sulfated polysaccharides from green seaweed udotea flabellum in cells exposed to oxidative damage. Marine Drugs. (2018) 16:135. 10.3390/md16040135
21.
HuangLHLiuHChenJYSunXYYaoZHHanJet al. Seaweed Porphyra yezoensis polysaccharides with different molecular weights inhibit hydroxyapatite damage and osteoblast differentiation of A7R5 cells. Food Funct. (2020) 11:3393–3409. 10.1039/C9FO01732A
22.
GuoYSunJYeJMaWYanHWangG. Saussurea tridactyla Sch. Bip.-derived polysaccharides and flavones reduce oxidative damage in ultraviolet B-irradiated HaCaT cells via a p38MAPK-independent mechanism. Drug Des Dev Ther. (2016) 10:389–403. 10.2147/DDDT.S96581
23.
WangLOhJYHwangJKoJYJeonYJRyuB. In vitro and in vivo antioxidant activities of polysaccharides isolated from celluclast-assisted extract of an edible brown seaweed, Sargassum fulvellum. Antioxidants. (2019) 8:493. 10.3390/antiox8100493
24.
CuiMZhouRWangYZhangMLiuKMaC. Beneficial effects of sulfated polysaccharides from the red seaweed Gelidium pacificum Okamura on mice with antibiotic-associated diarrhea. Food Funct. (2020) 11:4625–37. 10.1039/D0FO00598C
25.
KamelHNaviBBNakagawaKHemphillJC3rdKoNU. Hypertonic saline versus mannitol for the treatment of elevated intracranial pressure: a meta-analysis of randomized clinical trials. Crit Care Med. (2011) 39:554–9. 10.1097/ccm.0b013e318206b9be
26.
AnichiniCLottiFPietriniALo RizzoCLonginiMProiettiFet al. Antioxidant effects of potassium ascorbate with ribose in costello syndrome. Anticancer Res. (2013) 33:691–5. 10.1007/s10269-013-2254-1
27.
JiaBLYuanDPLanWJXuanYHJeonCO. New insight into the classification and evolution of glucose transporters in the Metazoa. FASEB J. (2019) 33:7519–28. 10.1096/fj.201802617R
28.
Kimoto-NiraHMoriyaNHayakawaSKuramasuKOhmoriHYamasakiSet al. Effects of rare sugar D-allulose on acid production and probiotic activities of dairy lactic acid bacteria. J Dairy Sci. (2017) 100:5936–44. 10.3168/jds.2016-12214
29.
JeongSCJeongYTLeeSMKimJH. Immune-modulating activities of polysaccharides extracted from brown algae Hizikia fusiforme. Biosci Biotechnol Biochem. (2015) 79:1362–5. 10.1080/09168451.2015.1018121
30.
TangTHeB. Treatment of D-galactose induced mouse aging with Lycium barbarum polysaccharides and its mechanism study. Afr J Tradit Complement Altern Med. (2013) 10:12–7. 10.4314/ajtcam.v10i4.3
31.
KsiazekAKonarzewskiMLapoIB. Anatomic and energetic correlates of divergent selection for basal metabolic rate in laboratory mice. Physiol Biochem Zool. (2004) 77:890–9. 10.1086/425190
32.
ManiniTM. Energy expenditure and aging. Ageing Res Rev. (2010) 9:1. 10.1016/j.arr.2009.08.002
33.
KhanSSSingerBDVaughanDE. Molecular and physiological manifestations and measurement of aging in humans. Aging Cell. (2017) 16:624–33. 10.1111/acel.12601
34.
KimHJPanJHKimSHLeeJHParkJW. Chlorogenic acid ameliorates alcohol-induced liver injuries through scavenging reactive oxygen species. Biochimie. (2018) 150:131–8. 10.1016/j.biochi.2018.05.008
35.
LiuXFanNWuLWuCZhouYLiPet al. Lighting up alkaline phosphatase in drug-induced liver injury using a new chemiluminescence resonance energy transfer nanoprobe. Chem Commun. (2018) 54:12479–82. 10.1039/C8CC07211F
36.
TessariP. Nitric oxide in the normal kidney and in patients with diabetic nephropathy. J Nephrol. (2015) 28:257–68. 10.1007/s40620-014-0136-2
37.
Abbasi HabashiSSabouniFMoghimiAAnsari MajdS. Modulation of lipopolysaccharide stimulated nuclear factor kappa B mediated iNOS/NO production by bromelain in rat primary microglial cells. Iran Biomed J. (2015) 20:33–40. 10.7508/ibj.2016.01.005
38.
ZhangZJCheangLCWangMWLeeSM. Quercetin exerts a neuroprotective effect through inhibition of the iNOS/NO system and pro-inflammation gene expression in PC12 cells and in zebrafish. Int J Mol Med. (2010) 27:195–203. 10.3892/ijmm.2010.571
39.
SiekierzyckaAStepnowskaMDobruckiLWWojciechowskiJWozniakMRogowskiJet al. Endothelial dysfunction in arteries from patients with induced hyperhomocysteinemia is associated with eNOS-mediated nitrooxidative stress. Eur Heart J. (2013) 34:5695. 10.1093/eurheartj/eht310.P5695
40.
BonthiusDJJrWintersZKaracayBBousquetSLBonthiusDJ. Importance of genetics in fetal alcohol effects: null mutation of the nNOS gene worsens alcohol-induced cerebellar neuronal losses and behavioral deficits. Neurotoxicology. (2015) 46:60–72. 10.1016/j.neuro.2014.11.009
41.
BalkeJEZhangLPercivalJM. Neuronal nitric oxide synthase (nNOS) splice variant function: insights into nitric oxide signaling from skeletal muscle. Nitric Oxide. (2019) 82:35–47. 10.1016/j.niox.2018.11.004
42.
DobutovicBSudarETepavcevicSDjordjevicJDjordjevicARadojcicMet al. Effects of ghrelin on protein expression of antioxidative enzymes and iNOS in the rat liver. Arch Med Sci. (2014) 10:806–16. 10.5114/aoms.2014.44872
43.
HuGItoORongRSakuyamaAMiuraTItoDet al. Pitavastatin upregulates nitric oxide synthases in the kidney of spontaneously hypertensive rats and Wistar-Kyoto rats. Am J Hypertens. (2018) 31:1139–1146. 10.1093/ajh/hpy098
44.
LaczaZSnipesJAZhangJHorváthEMFigueroaJPSzabóCet al. Mitochondrial nitric oxide synthase is not eNOS, nNOS or iNOS. Free Radic Biol Med. (2003) 35:1217–28. 10.1016/s0891-5849(03)00510-0
45.
ZhangJVeaseyS. Making sense of oxidative stress in obstructive sleep apnea: mediator or distracter?Front Neurol. (2012) 3:179. 10.3389/fneur.2012.00179
46.
LeeOHYoonKYKimKJYouSGLeeBY. Seaweed extracts as a potential tool for the attenuation of oxidative damage in obesity-related pathologies. J Phycol. (2011) 47:548–56. 10.1111/j.1529-8817.2011.00974.x
47.
La SalaLMrakic-SpostaSMicheloniSPrattichizzoFCerielloA. Glucose-sensing microRNA-21 disrupts ROS homeostasis and impairs antioxidant responses in cellular glucose variability. Cardiovas Diabetol. (2018) 17:105. 10.1186/s12933-018-0748-2
48.
VesentiniNBarsantiCMartinoAKusmicCRipoliARossiAet al. Selection of reference genes in different myocardial regions of an in vivo ischemia/reperfusion rat model for normalization of antioxidant gene expression. BMC Res Notes. (2012) 5:124. 10.1186/1756-0500-5-124
49.
KosenkoEATikhonovaLAAlilovaGAMontoliuCBarretoGEAlievGet al. Portacaval shunting causes differential mitochondrial superoxide production in brain regions. Free Radic Biol Med. (2017) 113:109–18. 10.1016/j.freeradbiomed.2017.09.023
50.
SelvaratnamJSRobaireB. Effects of aging and oxidative stress on spermatozoa of superoxide-dismutase 1- and catalase-null mice. Biol Reprod. (2016) 95:1–13. 10.1095/biolreprod.116.141671
51.
MaYFWuZHGaoMLoorJJ. Nuclear factor erythroid 2-related factor 2 antioxidant response element pathways protect bovine mammary epithelial cells against H2O2-induced oxidative damage in vitro. J Dairy Sci. (2018) 101:5329–44. 10.3168/jds.2017-14128
52.
BerndtCLilligCH. Glutathione, glutaredoxins, and iron. Antioxid Redox Signal. (2017) 27:1235–51. 10.1089/ars.2017.7132
53.
Vázquez-MedinaJPZenteno-SavínTFormanHJCrockerDEOrtiz1RM. Prolonged fasting increases glutathione biosynthesis in postweaned northern elephant seals. J Exp Biol. (2011) 214:1294–9. 10.1242/jeb.054320
54.
HosenMBIslamMRBegumFKabirYHowladerMZ. Oxidative stress induced sperm DNA damage, a possible reason for male infertility. Iran J Reprod Med. (2015) 13:525–32. 10.1007/s00192-007-0454-1
55.
HongCCaoJWuCFKadiogluOSchüfflerAKauhlUet al. The Chinese herbal formula Free and Easy Wanderer ameliorates oxidative stress through KEAP1-NRF2/HO-1 pathway. Sci Rep. (2017) 7:11551. 10.1038/s41598-017-10443-6
56.
DaiCTangSDengSZhangSZhouYVelkovTet al. Lycopene attenuates colistin-induced nephrotoxicity in mice via activation of the Nrf2/HO-1 pathway. Antimicrob Agents Chemother. (2014) 59:579–85. 10.1128/aac.03925-14
57.
IwayamaKKusakabeAOhtsuKNawanoTTatsunamiROhtakiKIet al. Long-term treatment of clarithromycin at a low concentration improves hydrogen peroxide-induced oxidant/antioxidant imbalance in human small airway epithelial cells by increasing Nrf2 mRNA expression. BMC Pharmacol Toxicol. (2017) 18:15. 10.1186/s40360-017-0119-8
58.
JiangXPTangJYXuZHanPQinZQYangCDet al. Sulforaphane attenuates di-N-butylphthalate-induced reproductive damage in pubertal mice: Involvement of the Nrf2-antioxidant system. Environ Toxicol. (2017) 32:1908–17. 10.1002/tox.22413
59.
MiaoJLShiHQJiangYHZhangBTHouXG. Studies on biochemical composition of Antarctic ice-microalgae and its relation to the cold acclimation. Adv Marine Sci. (2002) 20:43–50. 10.3969/j.issn.1671-6647.2002.04.007
60.
PletikapićGRadićTNZimmermannAHSvetličićVPfannkuchenMMarićDet al. AFM imaging of extracellular polymer release by marine diatom Cylindrotheca closterium (Ehrenberg) Reiman & J.C. Lewin. J Mol Recognit. (2011) 24:436–45. 10.1002/jmr.1114
Summary
Keywords
Antarctic ice microalgae, polysaccharide, D-galactose, oxidative damage, mice
Citation
Yi R, Deng L, Mu J, Li C, Tan F and Zhao X (2021) The Impact of Antarctic Ice Microalgae Polysaccharides on D-Galactose-Induced Oxidative Damage in Mice. Front. Nutr. 8:651088. doi: 10.3389/fnut.2021.651088
Received
08 January 2021
Accepted
16 February 2021
Published
09 March 2021
Volume
8 - 2021
Edited by
Miguel Angel Prieto Lage, University of Vigo, Spain
Reviewed by
Paula García Oliveira, Polytechnic Institute of Bragança (IPB), Portugal; María Carpena Rodríguez, Polytechnic Institute of Bragança (IPB), Portugal; Antía González Pereira, University of Vigo, Spain
Updates
Copyright
© 2021 Yi, Deng, Mu, Li, Tan and Zhao.
This is an open-access article distributed under the terms of the Creative Commons Attribution License (CC BY). The use, distribution or reproduction in other forums is permitted, provided the original author(s) and the copyright owner(s) are credited and that the original publication in this journal is cited, in accordance with accepted academic practice. No use, distribution or reproduction is permitted which does not comply with these terms.
*Correspondence: Xin Zhao zhaoxin@cque.edu.cnFang Tan tanfang@foods.ac.cn
This article was submitted to Food Chemistry, a section of the journal Frontiers in Nutrition
†These authors have contributed equally to this work
Disclaimer
All claims expressed in this article are solely those of the authors and do not necessarily represent those of their affiliated organizations, or those of the publisher, the editors and the reviewers. Any product that may be evaluated in this article or claim that may be made by its manufacturer is not guaranteed or endorsed by the publisher.