Bisphenol A (BPA) is an important industrial raw material. Because of its widespread use and increasing release into environment, BPA has become a new environmental pollutant. Previous studies about BPA’s effects in plants focus on a certain growth stage. However, the plant’s response to pollutants varies at different growth stages. Therefore, in this work, BPA’s effects in soybean roots at different growth stages were investigated by determining the reactive oxygen species levels, membrane lipid fatty acid composition, membrane lipid peroxidation and antioxidant systems. The results showed that low-dose BPA exposure slightly caused membrane lipid peroxidation but didn’t activate antioxidant systems at the seedling stage and this exposure did not affect above process at other growth stages; high-dose BPA increased reactive oxygen species levels and then caused membrane lipid peroxidation at all growth stages although it activated antioxidant systems and these effects were weaker with prolonging the growth stages. The recovery degree after withdrawal of BPA exposure was negatively related to BPA dose, but was positively related to growth stage. Taken together, the effects of BPA on antioxidant systems in soybean roots were associated with BPA exposure dose and soybean growth stage.
Bisphenol A [BPA; 2,2-bis (4-hydroxyphenyl)] is a chemical intermediate for synthesizing polycarbonate and epoxy1. It is widely applied in the production of daily necessities, such as baby bottles, food packaging, thermal paper, electronic equipment and medical facilities2,3. Recently, it was reported that the global annual output of BPA is up to 6.8 million tons4. The production and consumption of BPA are fairly stable in Europe, but in Asia, especially China, they are increasing gradually3. Due to the massive use and emissions of BPA products, BPA is widespread in the global environment. It was reported that BPA concentrations in surface water in the Netherlands and Germany are up to 21 μg·L−1 1 and 0.41 μg·L−1 5, respectively. In Japan, the concentration of BPA in garbage leachate is 17.2 mg·L−1 6. Toxicological studies on animals showed that BPA has estrogen activity that can disrupt physiological functions of animals and humans, especially in the reproductive and endocrine systems7,8,9.
Plants are the primary producers in ecological system and can provide organic materials and energy for secondary consumers. Through food chains in ecological systems, the hazards of BPA can extend to animals, even humans10. The European Union has released a risk assessment report of BPA on terrestrial ecosystems. The draft of the report requires researchers to focus on BPA toxicity on plants to further investigate the potential risks of BPA on plants11. Recently, the effects of BPA on algae have been frequently reported12,13, but the effects of BPA on terrestrial plants are less studied14 and the microscopic mechanism of BPA on plants remains unclear15. Previous studies showed that certain doses of BPA exposure could promote or inhibit the growth15,16, germination17, pollen tube elongation18, photosynthesis19 and hormone contents20 in plants. As a vital organ of plants in long-term adaptations to land, roots can absorb water and nutrients from soil for plant growth and development21 and roots also have the ability to absorb, fix and transfer pollutants. Compared to the aerial parts of plants, roots are directly exposed to BPA in the soil; thus, it is important to study the microscopic mechanisms of BPA on plant roots. Previous studies showed that 1.5 mg·L−1 BPA could promote glutamine synthetase/glutamate synthetase cycles and glutamate dehydrogenase pathways in soybean roots for the synthesis of amino acids and proteins, thereby promoting root growth22. However, 17.2 and 50.0 mg·L−1 BPA inhibit glutamine synthetase/glutamate synthetase cycles and promote glutamate dehydrogenase pathways, leading to the production of excessive amino acids and proteins, thus inhibiting root growth22.
Reactive oxygen species (ROS) are a type of oxidants, which include superoxide anion (O2−), hydrogen peroxide (H2O2) and hydroxyl radical (·OH). They have active chemical properties and strong oxidizability23,24. ROS are produced in aerobic metabolism in plants24. As signaling molecules, ROS can regulate metabolism in plant roots, thus affecting plant growth and development25. Plants have formed complete antioxidant systems (antioxidant enzymes and non-enzymatic substances) during long-term evolution processes to regulate ROS levels and to resist adversity stress. The antioxidant enzymes mainly include superoxide dismutase (SOD), peroxidase (POD) and catalase (CAT)26 and antioxidant non-enzymatic substances mainly include glutathione (GSH), proline (Pro) and ascorbic acid (AsA)27. Therefore, studying the effects of BPA on ROS levels and antioxidant systems in plant roots is important for understanding root function, growth and even the entire life status of plants.
Plant life cycles consist of different growth stages. The effects of the combined stress of soil acidification and lead ion on the antioxidant systems in soybean roots varies at different growth stages28. Unfortunately, the indicator systems used in previous studies on the environmental toxicology of BPA was relatively simple, or previous studies focused mainly on single growth stages in the plant life cycle15,16,22,28. Therefore, previous studies could not comprehensively, systematically and accurately reflect plant responses to BPA exposure, thus the results could mislead scientists working to objectively evaluate the ecological risk of BPA. In this study, the effects of BPA on ROS levels, membrane lipid fatty acids, membrane lipid peroxidation and antioxidant enzyme activities and non-enzymatic substance contents in soybean roots at different growth stages (seedling stage, flowering and podding stage, seed-filling stage) were investigated to evaluate whether there are differences among different growth stages. The results will provide new information to evaluate the microscopic mechanism of BPA on plants at all growth stages.
Effects of BPA on ROS levels and membrane lipid peroxidation in soybean roots at different growth stages
Figure 1 shows the effects of BPA on ROS levels and membrane lipid peroxidation in soybean roots at different growth stages. Compared to the control, after 7 d of 1.5 mg·L−1 BPA exposure, the H2O2 content at the seedling stage increased (p < 0.05), but the O2− and malondialdehyde (MDA) contents and membrane permeability did not change (p > 0.05) and those indices at both flowering and podding stages and seed-filling stages did not change (p > 0.05). With an increasing BPA dose (6.0 and 12.0 mg·L−1), the O2− content, MDA content and membrane permeability significantly increased (p < 0.05) at the three growth stages. Moreover, the increase degree of the O2− content and membrane permeability were positively related to the BPA dose, but negatively related to the growth stage. Moreover, the O2− content, MDA content and membrane permeability at the three growth stages did not change (p > 0.05) after withdrawal of 1.5 mg·L−1 BPA exposure, but increased (p < 0.05) after withdrawal of 6.0 and 12.0 mg·L−1 BPA exposure.
Effects of BPA on the composition of membrane lipid fatty acids in soybean roots at different growth stages
Tables 1, 2 and 3 show the effects of BPA on the composition of membrane lipid fatty acids in soybean roots at different growth stages. Compared to the control, after 7 d of 1.5 mg·L−1 BPA exposure, the composition of fatty acids at all growth stages did not change (p > 0.05), but the percentage content of different fatty acids changed (p < 0.05). The total contents of saturated fatty acids (SFA) increased (p < 0.05), whereas the total contents of unsaturated fatty acids (UFA) and the index of unsaturated fatty acids (IUFA) decreased (p < 0.05). After 7 d of 6.0 mg·L−1 BPA exposure, the SFA contents at the seedling stage as well as at the flowering and podding stage increased (p < 0.05), whereas the UFA content and IUFA decreased (p < 0.05). Moreover, only the IUFA at the seed-filling stage decreased (p < 0.05). After 12.0 mg·L−1 BPA exposure at different growth stages, the changes in all indices were similar to those after 6.0 mg·L−1 BPA exposure and the change degrees were positively related to the BPA dose but negatively related to the growth stage. After withdrawal of BPA exposure, the SFA contents increased (p < 0.05) at the seedling stage, while the UFA content and IUFA decreased (p < 0.05); the SFA and UFA content as well as the IUFA at the flowering and podding stages did not change obviously (p > 0.05). Interestingly, the SFA content at the seed-filling stage decreased (p < 0.05).
Effects of BPA on the activities of antioxidant enzymes in soybean roots at different growth stages
Figure 2 shows the effects of BPA on the activities of antioxidant enzymes in soybean roots at different growth stages. Compared to the control, after 1.5 mg·L−1 BPA exposure, the activities of SOD, POD and CAT at three growth stages did not change significantly (p > 0.05). After 6.0 mg·L−1 BPA exposure, the above indices increased (p < 0.05) at the seedling stage and the SOD and CAT activities at the flowering and podding stage and the seed-filling stage increased (p < 0.05). After 12.0 mg·L−1 BPA exposure, the activities of the three antioxidant enzymes at the three growth stages increased significantly (p < 0.05). After withdrawal of 1.5 mg·L−1 BPA exposure, the activities of the antioxidant enzymes at different growth stages did not change (p > 0.05); however, after withdrawal of 6.0 and 12.0 mg·L−1 BPA exposures, the activities of antioxidant enzymes at all growth stages increased (p < 0.05), except for the POD activity at the flowering and podding stage after withdrawal of 6.0 mg·L−1 BPA exposure.
Effects of BPA on the contents of antioxidant substances in soybean roots at different growth stages
Figure 3 shows the effects of BPA on the contents of antioxidant substances in soybean roots at different growth stages. Compared to the control, after 1.5 mg·L−1 BPA exposure, the Pro content at seedling stage increased (p < 0.05) and the contents of Pro, AsA and GSH at the flowering and podding stage and the seed-filling stage did not change (p > 0.05). With an increase in the BPA dose (6.0 and 12.0 mg·L−1), the contents of all antioxidant substances at different growth stages increased (p < 0.05). After withdrawal of 1.5 mg·L−1 BPA exposure, the changes in the content of antioxidant substances at the seedling stage were similar with those after this dose of BPA exposure. The Pro content recovered, but did not recover to the control levels; however, the content of antioxidant substances at the latter two growth stages had no significant changes (p > 0.05). After withdrawal of 6.0 and 12.0 mg·L−1 BPA exposures, the content of the antioxidant substances at each growth stage increased (p < 0.05).
Table 4 shows the relationship between antioxidant systems and ROS levels as well as membrane lipid peroxidation in soybean roots at different growth stages. At the seedling stage, after BPA exposure, H2O2 and MDA contents were positively correlated with antioxidant levels and O2− content and membrane permeability were positively related to the activities of antioxidant enzymes and GSH content, but the IUFA showed no correlation with antioxidant levels. After withdrawal of BPA exposure, the correlations between ROS levels and antioxidant levels were positive, except for the Pro content; the MDA content was positively correlated with the SOD activity; and the IUFA was negatively correlated with the CAT activity and Pro content. At the flowering and podding stage, after BPA exposure, those correlation relationships were similar to those at the seedling stage, but the IUFA showed a negative correlation with most antioxidant system indexes. After withdrawal of BPA exposure, the correlations were similar to those after BPA exposure. At the seed-filling stage, after BPA exposure, the correlations became more significant than those at the flowering and podding stage, but the IUFA still showed no correlation with antioxidant system levels. After withdrawal of BPA exposure, the correlations were similar to those after BPA exposure, except that the MDA content showed no correlation with antioxidant levels.
The production and removal of ROS in plants maintain a dynamic balance under normal conditions25. Under adversity, however, a large number of ROS (H2O2 and O2−) will be produced in plant cells, thus breaking the balance29. Our results showed that low dose of BPA (1.5 mg·L−1) exposure caused higher production of H2O2 than removal in soybean roots (Fig. 1) at the seedling stage and this imbalance was aggravated as BPA exposure dose increased (Fig. 1). After withdrawal of BPA exposure, the imbalance did not return to the control levels (Fig. 1). Excessive ROS can attack the polyunsaturated fatty acid in the cell membrane, causing membrane lipid peroxidation30 and an increase in membrane permeability. Moreover, excessive ROS can be used to generate more toxic ·OH by promoting the Fenton reaction31, affecting plant physiological activity and inhibiting plant growth and development29. MDA is a product of membrane lipid peroxidation; thus, the MDA content is an important index to evaluate the degree of membrane lipid peroxidation32. UFA is the main component of cell membrane lipids in organisms and it can regulate a variety of abiotic stresses in plants33. Low dose of BPA (1.5 mg·L−1) exposure led to excessive production of ROS in soybean roots at the seedling stage, causing oxidative stress to the UFA (Table 1), rather than membrane lipid peroxidation (Fig. 1). Higher doses of BPA exposure (6.0 and 12.0 mg·L−1) caused excessive accumulation of ROS, leading to the self-catalytic effect of free radical chain reactions aggravating the oxidation of the UFA (Table 1), finally causing decreases in membrane fluidity and membrane lipid peroxidation (Fig. 1). SOD is the first line of defense in plants to disproportionate O2− to H2O2. POD is an important enzyme in the cell walls or cytosol of plants and it can catalyze reactions from H2O2 to H2O to achieve detoxification34. CAT is in the peroxisome or mitochondria and its function is similar to that of POD, though CAT has a low substrate affinity34. AsA is an effective scavenger of free radicals and has antioxidant functions35 and the decrease in its levels indicates a decline in the total antioxidant capacity. As an antioxidant, GSH can directly remove ROS and at the same time, GSH itself can be oxidized to oxidized glutathione36. Pro regulates the osmosis of cell membranes and coordinates intracellular metabolic processes37. In this work, we found that low dose (1.5 mg·L−1) of BPA exposure caused oxidative stress to soybean roots at the seedling stage (Fig. 1) and the accumulation of Pro in cells to regulate cell membrane permeability and reduce the absorption of BPA by roots37, but this did not cause membrane lipid peroxidation or activate the antioxidant systems (Figs 1, 2, 3). High doses of BPA exposure activated the antioxidant enzyme systems to remove excess ROS (Table 1), while membrane lipid peroxidation was not avoided (Fig. 1 and Table 1). After withdrawal of high doses of BPA exposure, membrane lipid peroxidation did not disappear, indicating that the structure of soybean roots at the seedling stage did not develop well and stress resistance and self-healing abilities were relatively low38; thus, BPA exposure damaged the membrane structure of soybean seedling roots.
To objectively evaluate whether the effects of BPA on antioxidant systems in soybean roots varies at different growth stages, we also studied the effects of BPA exposure on antioxidant systems in roots at the flowering and podding stage and the seed-filling stage. The flowering and podding stage is the important period for soybean to alternately grow and reproduce, as well as a period for forming dry matter. Our results showed that low-dose BPA (1.5 mg·L−1) exposure did not significantly affect ROS levels, membrane lipid peroxidation or the antioxidant systems in soybean roots at the flowering and podding stage (Figs 1, 2, 3 and Table 2). This result indicates that the growth and metabolism of soybean at the flowering and podding stage are relatively strong and able to accumulate more biomass and the structure and function of roots are robust, which enables resilience to also be relatively strong37. The 6.0 mg·L−1 BPA exposure increased ROS levels and the increased ROS attacked polyunsaturated fatty acids in roots’ cell membranes, causing decreases in the UFA content (Table 2). Meanwhile, the activities of antioxidant enzymes and the levels of non-enzymatic substances increased to remove excess ROS (Figs 2 and 3). However, the increased ROS in soybean root cells was beyond the elimination abilities of antioxidant enzymes and non-enzymatic substances, leading to excessive accumulation of ROS and membrane lipid peroxidation (Fig. 1)30. Moreover, after withdrawal of BPA exposure, membrane lipid peroxidation did not disappear (Fig. 1), indicating that high-dose BPA exposure caused irreversible damage to soybean roots at the flowering and podding stage. At the same time, the antioxidant ability and ROS levels were positively correlated (Table 4), indicating that high doses of BPA exposure did not cause fatal damage to the antioxidant systems of soybean roots.
The seed-filling stage is the key period for the yield formation of soybean39. Previous studies showed that the growth, photosynthesis, nitrogen transfer and assimilation of soybean declined after entering the seed-filling stage40, but soybean roots still showed higher activities at late growth stages41. Our data suggested that the effects of BPA exposure on ROS levels, membrane lipid peroxidation and antioxidant systems in soybean roots at the seed-filling stage were similar to those at the flowering and podding stage (Figs 1, 2, 3 and Table 3) and the H2O2 content was higher than the O2− content (Fig. 1). We speculate that SOD constantly disproportionated O2− to H2O242 and that H2O2 is relatively stable and with greater longevity. Compared to the three growth stages, with the developing of soybean root structure and function and the increasing of biomass, BPA stress on unit biomass of soybean roots was decreased37. Previous studies showed that low-dose (1.5 mg·L−1) BPA exposure can promote roots to absorb and make use of microelements (such as Mg and Mn)43 and microelements can be used to synthesize antioxidants to resist ROS oxidative stress44. The resistance of soybean roots to BPA stress at three growth stages followed the order: seed-filling stage > flowering and podding stage > seedling stage. The effects of BPA on antioxidant systems at different growth stages in the entire soybean plant, including leaves, should be an area of future investigation.
In conclusion, the effects of BPA on ROS levels, membrane lipid peroxidation and antioxidant systems in soybean roots were aggravated with increasing BPA exposure dose but weaker with prolonging the growth stages. After withdrawal of BPA exposure, these effects became weaker and the recovery degree was negatively related to BPA exposure dose and positively related to growth stage.
Materials and Methods
Preparation of BPA solution
Given current global BPA pollution situation, especially in developing countries6,45, previous studies about the effects of BPA on plants and animals46,47,48 and high environmental levels of BPA released by pollution accident, three BPA doses (1.5, 6.0 and 12.0 mg·L−1) were selected. Of these concentrations, 1.5 mg·L−1 BPA is assigned by the United States Environmental Protection Agency as a safe dose for drinking water and the upper safety limit for individuals49 and this dose is often used to investigate the effects of BPA on plants17,47,49; 6.0 and 12.0 mg·L−1 are the BPA concentrations in soil, river sediment and hazardous landfill leachates50,51,52 and these two doses are also used to study the effects of BPA on plants53. Different doses of BPA solutions were prepared by dissolving suitable amounts of BPA in one-half strength Hoagland solution (pH 7.0).
Plant culture and BPA exposure
Soybean (Glycine max, Zhonghuang 25) seeds were germinated in accordance with previously reported methods19. Thirty days after germination, when there were both flowers and young raised pods (approximately 2 cm) in the soybean plants, the soybean plants were transplanted into BPA solutions at different doses (0.0, 1.5, 6.0 and 12.0 mg·L−1). The control plants were cultured in one-half strength Hoagland nutrient solution (pH 7.0) without BPA. Each treatment was performed 6 times. The BPA solution and the nutrient solution were renewed every 3 d. The plants were exposed to BPA solution for 7 d and then moved to one-half strength Hoagland solution (pH 7.0) without BPA for 7 d, based on our previous pre-experiment (in which the results showed that the effect of BPA on soybean seedling growth became steady after BPA exposure for 7 d and withdrawal of BPA exposure for another 7 d). After 7 d of BPA exposure, followed by 7 d of BPA withdrawal, the roots were collected for measurements of test indices.
Determination of ROS content and membrane lipid peroxidation
The H2O2 content in soybean roots was determined using a modification of a method described in previous reports54. Fresh roots (0.5 g) were homogenized in 3 mL of 50 mM potassium phosphate buffer (pH 6.5) at 4 °C and the homogenate was centrifuged at 11,500 × g for 15 min. The reaction mixture contained 3 mL supernatant and 1 mL of 20% H2SO4 (containing 0.1% TiCl4). The absorbance of the reaction mixture was determined at 410 nm and the H2O2 content was calculated by a standard curve.
The O2− content was determined according to previous methods37. Roots (2 g) were homogenized in 3 mL of 3% trichloroacetic acid and then the homogenate was centrifuged at 12,000 × g for 15 min. The reaction mixture contained 1 mL supernatant and 1 mL of 50 mM potassium phosphate buffer (pH 7.0, containing 1 mM hydroxylamine hydrochloride). The absorbance of the reaction mixture was recorded at 530 nm and the O2− content was calculated by the standard curve.
The MDA content was determined according to previous reports36. Roots (0.5 g) were collected and homogenized in 3 mL 1% trichloroacetic acid and the homogenate was centrifuged at 11,500 × g for 10 min. The reaction mixture contained 1 mL supernatant and 4 mL of 0.5% thiobarbituric acid and it was reacted in a boiling water bath for 30 min then quickly cooled in an ice bath. The reaction mixture was centrifuged again at 11,500 × g for 15 min. The absorbance of the supernatant was recorded at 450 nm, 532 nm and 600 nm. The concentration of MDA was calculated according to the following equation: Concentration (μmol·L−1) = 6.45 × (OD532 − OD600)−0.56 × OD450, where OD stands for optical density. The MDA content was expressed as nmol of MDA per g of fresh weight.
Membrane permeability was determined in accordance with previous methods, with slight modification55. Root fragments (0.5 g) were rinsed with deionized water and then put in glass tubes, which contained 10 mL deionized water. The roots were pumped in a vacuum environment for 20 min to translucent. The conductivity of the solution was measured with a conductivity meter (L1) and then the glass tubes were put in a boiling water bath to heat for 3–5 min. After being cooled to room temperature, the conductivity of the solution was measured again (L2). Membrane permeability was calculated using the followed formula: membrane permeability (E%) = (L1/L2) × 100%.
Determination of fatty acid composition
The extraction of total membrane lipids in soybean root cells was based on previous reports56. Soybean roots (1.0 g) were baked at 105 °C for 5 min, then the samples were homogenized in a mixture of chloroform and methanol (1:2, V: V) and the homogenate was centrifuged at 1,000 × g for 10 min. The mixture of the supernatant and 0.76% NaCl was oscillated for 15 min and then concentrated by nitrogen rotary evaporator to obtain total membrane lipids. Fatty acid composition was determined by gas chromatography57. Methanol (2 mL) and concentrated sulfuric acid (4–5 drops) were added into the total membrane lipid. The mixture was put in a water bath (50–60 °C) for 10 min then added into n-hexane (1–2 mL). After shock, the mixture stood for 15 min and 2 mL of distilled water were then added. The solvent in the supernatant was evaporated using nitrogen, after which the residues were analyzed using a Shimadzu GC-2010 gas chromatograph to automatically determine the sample. Standard substances of fatty acids were purchased from Sigma Company. The fatty acid content was obtained through comparisons with the peak area of the standard samples using quantitative analysis.
Determination of antioxidant enzymes activity
Fresh soybean roots (0.5 g) were collected and homogenized in a 50 mM phosphate buffer (pH 7.8), which contained 5 mM ascorbic acid, 5 mM dithiothreitol, 5 mM EDTA and 2% (v/v) polyvinylpyrrolidone. The homogenates were centrifuged at 15,000 × g for 15 min and the supernatant was used to determine the antioxidant enzyme activity.
The SOD activity was determined using a modified method based on previous reports36. The mixture reacted under fluorescent lights for 30 min. One unit of enzyme activity was defined as the quantity of SOD required for 50% inhibition of nitroblue tetrazolium reduction at 560 nm.
The POD activity was determined in accordance with previously reported methods with slight modification58. The reaction mixture (3 mL) contained 1 mL 25 mM phosphate buffer (pH 6.8), 5 μL 28 mM guaiacol and 15 μL enzyme extract. A few drops of H2O2 were added to initiate reaction and one unit of enzyme activity was defined as the change of absorbance at 470 nm within 1 min.
The determination of the CAT activity was based on previous reports59. The reaction mixture (3 mL) contained 100 mM phosphate buffer (pH 7.0) and 50 μL of enzyme extract. The 15 mM H2O2 (a few drops) was added into the mixture to initiate reaction. One unit of enzyme activity was defined as the decomposition of H2O2 (mg) from a fresh sample (g) at 240 nm within 1 min.
Determination of the contents of non-enzymatic antioxidant substance
The AsA content was determined according to previous reports37. Roots (0.5 g) were homogenized in 5% trichloroacetic acid. Then, the homogenate was centrifuged at 4,000 × g for 10 min. The reaction mixture contained 0.2 mL supernatant, 0.5 mL of 150 mM phosphate buffer (pH 7.4, containing 5 mM EDTA) and 0.2 mL deionized water. The reaction mixture was incubated at 40 °C for 40 min and the absorbance was recorded at 532 nm. The AsA content was calculated by the standard curve.
The determination of the Pro content was carried out according to previous reports with slight modifications36. Roots (0.5 g) were collected and homogenized in 10 mL of 3% sulfosalicylic acid. Then, the homogenate was centrifuged at 1,000 × g for 10 min. The mixture (containing 2 mL supernatant, 2 mL ice acetic acid and 4 mL 2.5% ninhydrin) underwent a reaction in a 100 °C water bath for 40 min and then was rapidly cooled to terminate the reaction. The absorbance was recorded at 520 nm and the Pro content was calculated by the standard curve.
The GSH content was determined in accordance with previously reported methods36. Roots (0.5 g) were collected and homogenized in 5 mL of 0.1 M HCl (pH 2.0) and the homogenate was centrifuged at 10,000 × g at 4 °C for 10 min. The reaction mixture contained 200 μL supernatant, 800 μL of 0.5 M KH2PO4/K2HPO4 buffer (pH 8.0), a few drops of 1 mM EDTA and 100 μL of 6 mM 5, 5-dithiobis-(2-nitrobenzoic acid) (Sigma, USA). The mixture was reacted at 30 °C in a water bath for 15 min. The absorbance was determined at 412 nm and the GSH content was calculated by standard curve.
Each treatment group was set up 6 times and all data for the three independent experiments of the mean value ± standard error (mean ± SD). The significant differences (p < 0.05) between the different treatments were analyzed using an LSD test with SPSS 17.0 software. The symmetric quantitative variables were used to calculate the Pearson’s correlation coefficient and to perform correlation analysis among test indices.
How to cite this article: Zhang, J. et al. Analysis of effects of a new environmental pollutant, bisphenol A, on antioxidant systems in soybean roots at different growth stages. Sci. Rep. 6, 23782; doi: 10.1038/srep23782 (2016).
Belfroid, A., van Velzen, M., van der Horst, B. & Vethaak, D. Occurrence of bisphenol A in surface water and uptake in fish: evaluation of field measurements. Chemosphere 49, 97–103 (2002).
Staples, C. A., Dorn, P. B., Klecka, G. M., O’Block, S. T. & Harris, L. R. A review of the environmental fate, effects and exposures of bisphenol A. Chemosphere 36, 2149–2173 (1998).
Huang, Y. Q. et al. Bisphenol A (BPA) in China: a review of sources, environmental levels and potential human health impacts. Environ. Int. 42, 91–99 (2012).
Jandegian, C. M. et al. Developmental exposure to bisphenol A (BPA) alters sexual differentiation inpainted turtles (Chrysemys picta). Gen. Comp. Endocrinol. 216, 77–85 (2015).
Fromme, H. et al. Occurrence of phthalates and bisphenol A and F in the environment. Water Res. 36, 1429–1438 (2002).
Yamamoto, T., Yasuhara, A., Shiraishi, H. & Nakasugi, O. Bisphenol A in hazardous waste landfill leachates. Chemosphere 42, 415–418 (2001).
Crain, D. A. et al. An ecological assessment of bisphenol-A: evidence from comparative biology. Reprod. Toxicol. 24, 225–239 (2007).
Liu, Y. et al. Acute toxicity of nonylphenols and bisphenol A to the embryonic development of the abalone Haliotis diversicolor supertexta. Ecotoxicology 20, 1233–1245 (2011).
Rhee, J. et al. Bisphenol A modulates expression of sex differentiation genes in the self-fertilizing fish, Kryptolebias marmoratus. Aquat. Toxicol. 104, 218–229 (2011).
Jondeau-Cabaton, A. et al. Characterization of endocrine disruptors from a complex matrix using estrogen receptor affinity columns and high performance liquid chromatography-high resolution mass spectrometry. Environ. Sci. Pollut. R. 20, 2705–2720 (2013).
European Commision. Updated European risk assessment report 4,4′ isopropylidenediphenol (bisphenol-A). Brussels (2008). Available at: http://publications.jrc.ec.europa.eu/repository/handle/JRC59980 (Accessed: 4th November 2010).
Ji, M. et al. Biodegradation of bisphenol A by the freshwater microalgae Chlamydomonas mexicana and Chlorella vulgaris. Ecol. Eng. 73, 260–269 (2014).
Zhang, W. et al. Acute and chronic toxic effects of bisphenol A on Chlorella pyrenoidosa and Scenedesmus obliquus. Environ. Toxicol. 29, 714–722 (2014).
Zhang, J. et al. Effects of bisphenol A on chlorophyll fluorescence in five plants. Environ. Sci. Pollut. R. 22, 17724–17732 (2015).
Qiu, Z., Wang, L. & Zhou, Q. Effects of bisphenol A on growth, photosynthesis and chlorophyll fluorescence in above-ground organs of soybean seedlings. Chemosphere 90, 1274–1280 (2013).
Sun, H., Wang, L. & Zhou, Q. Effects of bisphenol A on growth and nitrogen nutrition of roots of soybean seedlings. Environ. Toxicol. Chem. 32, 174–180 (2013).
Dogan, M., Korkunc, M. & Yumrutas, O. Effects of bisphenol A and tetrabromobisphenol A on bread and durum wheat varieties. Ekoloji 21, 114–122 (2012).
Speranza, A., Crosti, P., Malerba, M., Stocchi, O. & Scoccianti, V. The environmental endocrine disruptor, bisphenol A, affects germination, elicits stress response and alters steroid hormone production in kiwifruit pollen. Plant Biol. 13, 209–217 (2011).
Jiao, L. et al. Effects of bisphenol A on chlorophyll synthesis in soybean seedlings. Environ. Sci. Pollut. R. 22, 5877–5886 (2015).
Wang, S. et al. Effects of bisphenol A, an environmental endocrine disruptor, on the endogenous hormones of plants. Environ. Sci. Pollut. R. 22, 17653–17662 (2015).
Wang, H., Inukai, Y. & Yamauchi, A. Root development and nutrient uptake. Crit. Rev. Plant Sci. 25, 279–301 (2006).
Sun, H., Wang, L. H., Zhou, Q. & Huang, X. H. Effects of bisphenol A on ammonium assimilation in soybean roots. Environ. Sci. Pollut. R. 20, 8484–8490 (2013).
Cordeiro, R. M. Molecular dynamics simulations of the transport of reactive oxygen species by mammalian and plant aquaporins. BBA-Gen. Subjects. 1850, 1786–1794 (2015).
Karkonen, A. & Kuchitsu, K. Reactive oxygen species in cell wall metabolism and development in plants. Phytochemistry 112, 22–32 (2015).
Gao, Y.-B. et al. Low temperature inhibits pollen tube growth by disruption of both tip-localized reactive oxygen species and endocytosis in Pyrus bretschneideri Rehd. Plant Physiol. Bioch. 74, 255–262 (2014).
Wang, Z. et al. The effect of exogenous salicylic acid on antioxidant activity, bioactive compounds and antioxidant system in apricot fruit. Sci. Hortic-Amsterdam. 181, 113–120 (2015).
Ramakrishna, B. & Rao, S. S. R. Foliar application of brassinosteroids alleviates adverse effects of zinc toxicity in radish (Raphanus sativus L.) plants. Protoplasma 252, 665–677 (2015).
Wang, L., Wang, Q., Zhou, Q. & Huang, X. Combined effect of soil acidification and lead ion on antioxidant system in soybean roots. Chem. Ecol. 31, 123–133 (2015).
Ahmad, P., Sarwat, M. & Sharma, S. Reactive oxygen species, antioxidants and signaling in plants. J. Plant Biol. 51, 167–173 (2008).
Parlak, K. U. & Yilmaz, D. D. Response of antioxidant defences to Zn stress in three duckweed species. Ecotox. Environ. Safe. 85, 52–58 (2012).
Smith, B. A., Teel, A. L. & Watts, R. J. Identification of the reactive oxygen species responsible for carbon tetrachloride degradation in modified Fenton’s systems. Environ. Sci. Technol. 38, 5465–5469 (2004).
Jemec, A., Tisler, T., Erjavec, B. & Pintar, A. Antioxidant responses and whole-organism changes in Daphnia magna acutely and chronically exposed to endocrine disruptor bisphenol A. Ecotox. Environ. Safe. 86, 213–218 (2012).
Sui, N. & Han, G. Salt-induced photoinhibition of PSII is alleviated in halophyte Thellungiella halophila by increases of unsaturated fatty acids in membrane lipids. Acta. Physiol. Plant 36, 983–992 (2014).
Xu, C., Natarajan, S. & Sullivan, J. H. Impact of solar ultraviolet-B radiation on the antioxidant defense system in soybean lines differing in flavonoid contents. Environ. Exp. Bot. 63, 39–48 (2008).
Liu, F. et al. Higher transcription levels in ascorbic acid biosynthetic and recycling genes were associated with higher ascorbic acid accumulation in blueberry. Food Chem. 188, 399–405 (2015).
Du, S. et al. Atmospheric application of trace amounts of nitric oxide enhances tolerance to salt stress and improves nutritional quality in spinach (Spinacia oleracea L.). Food Chem. 173, 905–911 (2015).
Wang, Q. et al. Effects of bisphenol A on antioxidant system in soybean seedling roots. Environ. Toxicol. Chem. 34, 1127–1133 (2015).
Malekzadeh, P. Influence of exogenous application of glycinebetaine on antioxidative system and growth of salt-stressed soybean seedlings (Glycine max L.). Physiol. Mol. Biol. Plants 21, 225–232 (2015).
Kumudini, S. V., Pallikonda, P. K. & Steele, C. Photoperiod and e-genes influence the duration of the reproductive phase in soybean. Crop Sci. 47, 1510–1517 (2007).
Kaschuk, G., Hungria, M., Leffelaar, P. A., Giller, K. E. & Kuyper, T. W. Differences in photosynthetic behaviour and leaf senescence of soybean (Glycine max L. Merrill) dependent on N2 fixation or nitrate supply. Plant Biol. 12, 60–69 (2010).
Afza, R., Hardarson, G., Zapata, F. & Danso, S. K. A. Effects of delayed soil and foliar N fertilization on yield and N2 fixation of soybean. Plant Soil 97, 361–368 (1987).
Ahuja, N., Singh, H. P., Batish, D. R. & Kohli, R. K. Eugenol-inhibited root growth in Avena fatua involves ROS-mediated oxidative damage. Pestic. Biochem. Phys. 118, 64–70 (2015).
Nie, L. et al. Effects of bisphenol A on mineral nutrition in soybean seedling roots. Environ. Toxicol. Chem. 34, 133–140 (2015).
Sun, Z., Wang, L., Zhou, Q. & Huang, X. Effects and mechanisms of the combined pollution of lanthanum and acid rain on the root phenotype of soybean seedlings. Chemosphere 93, 344–352 (2013).
Goodson, A., Summerfield, W. & Cooper, I. Survey of bisphenol A and bisphenol F in canned foods. Food. Addit. Contam. 19, 796–802 (2002).
Mandich, A. et al. In vivo exposure of carp to graded concentrations of bisphenol A. Gen. Comp. Endocr. 153, 15–24 (2007).
Mihaich, E. M. et al. Acute and chronic toxicity testing of bisphenol A with aquatic invertebrates and plants. Ecotoxicol. Environ. Safe 72, 1392–1399 (2009).
Saiyood, S., Inthorn, D., Vangnai, A. S. & Thiravetyan, P. Phytoremediation of bisphenol A and total dissolved solids by the mangrove plant, Bruguiera gymnorhiza. Int. J. Phytoremediat. 15, 427–438 (2013).
Geens, T., Goeyens, L. & Covaci, A. Are potential sources for human exposure to bisphenol-A overlooked? Int. J. Hyg. Environ. Health. 214, 339–347 (2011).
Yamada, K., Urase, T., Matsuo, T. & Suzuki, N. Constituents of organic pollutants in leachates from different types of landfill sites and their fate in the treatment processes. J. Jpn. Soc. Phys. Water Environ. 22, 40–45 (1999).
Yasuhara, A. et al. Determination of organic components in leachates from hazardous waste disposal sites in Japan by gas chromatography–mass spectrometry. J. Chromatogra. A 774, 321–332 (1997).
Sun, W. L., Ni, J. R., O’Brien, K. C., Hao, P. P. & Sun, L. Y. Adsorption of bisphenol A on sediments in the Yellow River. Water Air Soil Poll. 167, 353–364 (2005).
Li, R. et al. Physiological responses of the alga Cyclotella caspia to bisphenol A exposure. Bot. Mar. 51, 360–369 (2008).
Hossain, M. A., Hasanuzzaman, M. & Fujita, M. Up-regulation of antioxidant and glyoxalase systems by exogenous glycinebetaine and proline in mung bean confer tolerance to cadmium stress. Physiol. Mol. Biol. Plants 16, 259–272 (2010).
Alpaslan, M. & Gunes, A. Interactive effects of boron and salinity stress on the growth, membrane permeability and mineral composition of tomato and cucumber plants. Plant Soil 236, 123–128 (2001).
Bligh, E. G. & Dyer, W. J. A rapid method of total lipid extraction and purification. Can. J. Biochem. Phys. 37, 911–917 (1959).
Harwood, J. Gas chromatography and lipids: a practical guide: by W. W. Christie, the oily press, Ayr, Scotland. Phytochemistry 28, 3251–3252 (1989).
Saba, M. K., Arzani, K. & Barzegar, M. Postharvest polyamine application alleviates chilling injury and affects apricot storage ability. J. Agr. Food. Chem. 60, 8947–8953 (2012).
Shi, S. Y., Wang, G., Wang, Y. D., Zhang, L. G. & Zhang, L. X. Protective effect of nitric oxide against oxidative stress under ultraviolet-B radiation. Nitric. Oxide-Biol. Ch. 13, 1–9 (2005).
The authors are grateful for the financial support provided by the Natural Science Foundation of China (21371100, 31170477), National Water Pollution Control and Management Technology Major Project (2012ZX07101_013), the Natural Science Foundation of Jiangsu Province (BK2011160), the Project Funded by the Priority Academic Program Development of Jiangsu Higher Education Institutions and Research and Innovation Project for Postgraduate of Higher Education Institutions of Jiangsu Province in 2015 (KYLX15_1189).
The authors declare no competing financial interests.
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Zhang, J., Li, X., Zhou, L. et al. Analysis of effects of a new environmental pollutant, bisphenol A, on antioxidant systems in soybean roots at different growth stages. Sci Rep 6, 23782 (2016). https://doi.org/10.1038/srep23782
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