Next Article in Journal
Signal-to-Noise Ratio Enhancement of Single-Voxel In Vivo 31P and 1H Magnetic Resonance Spectroscopy in Mice Brain Data Using Low-Rank Denoising
Previous Article in Journal
Metabolomic Analysis of Renal Cell Carcinoma in the Prostate, Lung, Colorectal, and Ovarian Cancer Screening Trial
 
 
Search for Articles:
Title / Keyword
Author / Affiliation / Email
Journal
Article Type
 
 
Advanced Search
 
Section
Special Issue
Volume
Issue
Number
Page
 
Journals
Metabolites
Volume 12
Issue 12
10.3390/metabo12121190
metabolites-logo
Submit to this Journal Review for this Journal Propose a Special Issue
► Article Menu

Article Menu

share Share announcement Help format_quote Cite question_answer Discuss in SciProfiles thumb_up
...
Endorse textsms
...
Comment
first_page
settings
Order Article Reprints
Font Type:
Arial Georgia Verdana
Font Size:
Aa Aa Aa
Line Spacing:
Column Width:
Background:
Article

Drought-Induced Xylem Sulfate Activates the ABA-Mediated Regulation of Sulfate Assimilation and Glutathione Redox in Brassica napus Leaves

by
Bok-Rye Lee
1,2,
Sang-Hyun Park
1,
Van Hien La
1,3,
Dong-Won Bae
4 and
Tae-Hwan Kim
1,*
1
Grassland Science Laboratory, Department of Animal Science, Institute of Agricultural Science and Technology, College of Agriculture & Life Science, Chonnam National University, Gwangju 61186, Republic of Korea
2
Institute of Environmentally-Friendly Agriculture (IEFA), Chonnam National University, Gwangju 61186, Republic of Korea
3
Center of Crop Research for Adaption to Climate Change (CRCC), Thai Nguyen University of Agriculture and Forestry, Thai Nguyen 24000, Vietnam
4
Biomaterial Analytical Laboratory, Central Instruments Facility, Gyeongsang National University, Jinju 52828, Republic of Korea
*
Author to whom correspondence should be addressed.
Metabolites 2022, 12(12), 1190; https://doi.org/10.3390/metabo12121190
Submission received: 14 October 2022 / Revised: 13 November 2022 / Accepted: 25 November 2022 / Published: 29 November 2022
(This article belongs to the Topic Plant Metabolism under Stress)
Browse Figures
Versions Notes

Abstract

:
Drought intensity modifies the assimilatory pathway of glutathione (GSH) synthesis. Abscisic acid (ABA) is a representative signaling hormone involved in regulating plant stress responses. This study aimed to investigate an interactive regulation of sulfate and/or ABA in GSH metabolism and redox. The drought-responsive alterations in sulfate assimilation and GSH-based redox reactions were assessed relative to ABA responses on the time-course of drought intensity. Drought-responsive H2O2 concentrations were divided into two distinct phases—an initial 4 days of no change (Ψw ≥ −0.49 MPa) and a phase of higher accumulation during the late phase of the drought (days 10–14; Ψw ≤ −1.34 MPa). During the early phase of the drought, GSH/GSSG redox state turned to the slightly reduced state with a transient increase in GSH, resulting from a strong activation of H2O2 scavenging enzymes, ascorbate peroxidase (APOX) and glutathione reductase (GR). The late phase of the drought was characterized by a decrease in GSH due to cysteine accumulation, shifting GSH- and NADPH-based redox states to higher oxidization, increasing sulfate and ABA in xylem, and causing ABA accumulation in leaves. Regression analysis revealed that sulfate in xylem sap was positively correlated with H2O2 concentrations and ABA was closely related to decreases in the GSH pool and the oxidation of GSH catalyzed by glutathione peroxidase (GPOX). These results indicate that drought-induced oxidation proceeds through the suppression of GSH synthesis and further GSH oxidation in a sulfate-activated ABA-dependent manner.

1. Introduction

Drought is the most common adverse environmental stress that limits plant growth and development in worldwide. In Korea, oilseed rape (Brassica napus L.) is often exposed to drought stress during the early stages of its growth since drought occurs predominantly from March to early June, which is the active growth and development period of most winter plant varieties. Decreasing water availability during droughts generally results in reduced total nutrient uptake, leading to reduced concentrations of mineral nutrients in plants. Sulfur (S) deficiency in plant cells reduces chlorophyll and Rubisco content and promotes chlorosis in young leaves [1,2,3], resulting in a general inhibition of photosynthesis and protein synthesis [4]. Thus, S-use efficiency has proven to be a significant determinant of drought-stress tolerance, specifically regarding photosynthetic activity in oilseed rape cultivars [4]. The closure of stomata triggered by drought results in a rapid decline of the plant’s internal CO2/O2 ratio, inducing a high flux of reactive oxygen species (ROS) production in the peroxisomes through photorespiration [5,6]. Among ROS, low steady-state levels of H2O2 function as signal transduction molecules [7,8]. However, excessive ROS becomes deleterious and results in oxidative damage to membranes (i.e., lipid peroxidation), proteins, RNA, and DNA in a process termed “oxidative stress” [5,9,10]. Subsequent studies have focused on disequilibrium in the cellular reduction–oxidation status, called “redox” status, as a cause of oxidative stress. S metabolism is an essential in the regulation of cellular redox homeostasis under stress; for example, thiol-containing compounds, especially reduced GSH (sensitive to oxidized environments), can be modulators of the stress response [11,12]. H2O2 is reduced to H2O by ascorbate, while reduced GSH is converted to glutathione disulfide (GSSG) upon oxidation with two other GSH molecules [13]. The resultant oxidized glutathione (GSSG) is recycled back to GSH by the action of glutathione reductase (GR), using NADPH as the reductant [14,15], thereby maintaining the redox potential of GSH. Although GSH, which depends on the availability of S assimilates from sulfate reduction pathway (especially cysteine), is an essential regulator in stress response and tolerance [11,16,17], the sulfate assimilation pathway towards GSH-based redox in response to drought-induced oxidative stress has rarely been investigated.
Several studies have provided evidence for significant co-regulation between S metabolism and abscisic acid (ABA) biosynthesis that highlights the importance of S for stress tolerance [18,19,20]. ABA is a well-characterized signaling molecule that induces stomatal closure [19,20] and stress symptomatic responses [6,8,21], along with stress-induced ROS accumulation. Sulfate has been shown to promote ABA synthesis [20] and sulfate–ABA interactions lead to a greater reduction in transpiration rates and stomatal aperture than ABA alone [18]. Studies have shown that sulfate is a xylem-born chemical signal as ABA synthesis and is transported earlier than ABA [18,22]. Exogenous sulfate- or cysteine (Cys) up-regulates the expression of the 9-sis-epoxycarotenoid dioxygenase (NCED3), which is a key step during ABA synthesis [20,22]. Furthermore, sulfate assimilation into Cys is required to trigger ABA biosynthesis and stomatal closure [19] and ABA-triggered stomatal closure is a result of Cys accumulation and is not influenced by lowered GSH [23,24]. Taken together, previous studies have provided evidence for an interactive biological function between sulfate and ABA involved in regulating stress responses and stress tolerance in vascular plants. However, little understanding has been developed in relation to how sulfate or S-assimilates regulate GSH-based redox in possible interactions with ABA as being linked to drought-induced H2O2 accumulation.
In the present study, we hypothesized that (1) the endogenous levels of sulfate assimilates and ABA in shoots, roots, as well as in xylem sap are greatly influenced by drought intensity-responsive endogenous H2O2 levels, and (2) the interconnected signaling and metabolic pathways between sulfate and ABA are involved in GSH-based redox control. To test these hypotheses, endogenous ABA, sulfate and S- assimilates, antioxidative enzymes activity, xylem-borne sulfate and ABA were assessed in relation to endogenous H2O2 levels in Brassica napus leaves, based on the time-course of drought intensity.

2. Materials and Methods

2.1. Plant Growth and Treatments

Brassica napus L. (cv. Capitol) seeds were sown in bed soil in a tray. When the plants reached the four-leaf stage, seedlings were transferred to 2 L pots containing a mixture of soil and perlite (70:30, w/w) inside a greenhouse. A complete nutrient solution was continuously supplied to the plants [25] and metal halide lamps (c. 400 μmol photons m−2 s−1 at the canopy for 6 h per day) were used to supply natural light. Plants were selected according to morphological similarities after 6 weeks and were divided into two groups, one that was irrigated with 200 mL of water for well-watered plants (control) and the other that was irrigated with 20 mL of water for drought-stressed plants. Sampling was performed consecutively at 0, 2, 4, 10 and 14 days after the drought treatment.

2.2. Measurement of Leaf Water Potential

For measurement of leaf water potential (Ψw), the seventh leaf was cut and placed in the pressure chamber (PMS Instruments, Corvallis, OR, USA) to expose the cut end of the petiole to the outside. Subsequently, pressure was applied to the chamber until liquid was observed at the end of the petiole, which corresponds to the Ψw.

2.3. Collection of Xylem and Phloem

Xylem samples were obtained by cutting stems. After thorough washing of the stem’s surface, the exuding fluid was collected under high pressure using an exhausted syringe. Phloem exudates were collected in accordance with the methods described by Lee et al. [10]. The petiole of the leaf rank number of 3 (i.e., leaf No. 1 was the oldest leaf) was cut and immersed rapidly in 20 mL of EDTA solution (pH 7.0) for 5 min. The leaf was rinsed, transferred to another 15 mL of 5 mM EDTA solution (pH 7.0), and maintained for 6 h in a growth chamber with 95% relative humidity in darkness. The resulting collection of fluid samples was stored at −80 °C for further analysis.

2.4. Measurement of H2O2 Concentration

To determine H2O2 concentrations, approximately 200 mg of well-ground fresh leaves were homogenized with 1.2 mL of 100 mM phosphate buffer (pH 7.0) and the mixture was then centrifuged at 10,000× g for 10 min. The resulting extract (0.2 mL) was mixed with 0.2 mL of 0.1% titanium chloride in 20% (v/v) H2SO4 and was then centrifuged at 6000× g for 3 min. Absorbance was immediately read at 410 nm and the H2O2 concentration calculated from the extinction coefficient was found to be 0.28 μM−1 cm−1 [26].

2.5. Determination of ABA Concentration

Quantitative analysis of ABA in leaves, roots and xylem was performed according to the protocol used by La et al. [27]. Briefly, 50 mg of fresh ground tissues and 50 μL of concentrated xylem were extracted with 500 μL of extraction solvent (2-propanol/H2O/concentrated HCl; 5:1:0.002, v/v/v) containing d6-ABA as the internal standard for ABA. Dichloromethane (1 mL) was added to the supernatant and then centrifuged at 13,000× g for 5 min at 4 °C. The lower phase, which was taken into a clean screw-cap glass vial, was dried under nitrogen and resolved in pure methanol. Complete dissolved extract was ensured by vortexing and sonicating was transferred to a reduced volume liquid chromatography vial. The level of ABA was measured using a reverse-phase C18 Gemini high-performance liquid chromatography (HPLC) column for HPLC electrospray ionization tandem mass spectrometry (HPLC–ESI–MS/MS) analysis. Agilent 1100 HPLC (Agilent Technologies, Waldbronn, Stuttgart, Germany), Waters C18 column (150 × 2.1 mm, 51 μm), and API4000 MSMRM (Applied Biosystems, Waltham, MA, USA) were used for analysis.

2.6. Sulfate and Cys Concentration

To measure the concentration of sulfate, approximately 100 mg of leaves and roots was homogenized with 1.5 mL of extraction buffer containing 1.8 mM Na2CO3 and 1.7 mM NaHCO3 (v/v = 1:1). Samples were centrifuged at 12,000× g for 10 min, after which the supernatant was filtered through a 0.2-μm membrane-type filter, as well as concentrated xylem. Sulfate concentrations were determined by using ion chromatography (Dionex, DX-120, Sunnyvale, CA, USA), using an isocratic Na2CO3/NaHCO3 eluent (1.8 mM/1.7 mM) with a flow rate of 2.3 mL min−1. To determine the Cys content within plant tissue, approximately 200 mg of freshly ground samples was extracted using 1 mL of Na-PO4 (pH 7.5). The aliquot was then isolated and added to an acid ninhydrin solution (i.e., 0.25 g of acid ninhydrin mixed with 6 mL of acetic acid and 4 mL of concentrated HCl), after which it was heated at 100 °C for 10 min and was then cooled in ice. The absorbance was determined at 560 nm and Cys content was calculated using a standard curve [28].

2.7. Measurement of GSH/GSSG

For total GSH extraction, 200 mg of fresh leaves were homogenized in a 5% solution of 5-sulfosalicylic acid and centrifuged at 12,000× g for 10 min. GSSG sample were prepared by adding a thiol scavenger (GT40c, Oxford Biomedical Research Inc., Rochester Hills, MI, USA) immediately to the total GSH-extracted solution. The total GSH and GSSG contents of the resulting supernatants were then determined through a microplate assay using the GSH/GSSG Kit GT40 (Oxford Biomedical Research Inc., Rochester Hills, MI, USA). The extracted solution for total GSH and GSSG were mixed with glutathione reductase, DTNB (5,5-dithiobisnitrogenzoic acid) and NADPH. The absorbance was immediately recorded at 405 nm by taking readings every minute for 10 min. Total GSH and GSSG concentration were calculated using standard curve of GSH and GSSG, respectively. GSH concentration was obtained by subtracting GSSG from total GSH.

2.8. Measurement of NADPH/NADP+

The contents of oxidized and reduced pyridine nucleotides were measured as described previously [27]. For NADP+ and NADPH extraction, 200 mg of fresh leaves were homogenized with 0.8 mL of 0.2 N HCl and 0.2 M NaOH, respectively; 100 mL of this extract was heated at 95 °C for 1 min and was then placed in an ice-bath. For the NADP+ assay, the supernatant was neutralized with 0.2 M NaOH to a final pH of 5–6, while NADPH was neutralized by 0.2 N HCl to a final pH of 7–8 for the NADPH assay. Forty microliters were added to the reaction mixture containing 0.1 M HEPES (pH 7.5), which consisted of 2 mM Na2EDTA, 1.2 mM dichlorophenolindophenol, 20 mM phenazine methosulfate, and 10 mM glucose-6-phosphate for NADPH/NADP+. The reaction was started by adding 2 μL of glucose 6-phosphate dehydrogenase (200 U) for NADPH/NADP+ and the content of NADP+ and NADPH were quantified using a standard curve.

2.9. Measurements of Antioxidant Enzyme Activities

Well-ground leaves were extracted with 100 mM of potassium phosphate buffer (pH 7.5) containing 2 mM of ethylenediaminetetraacetic acid, 1% polyvinylpyrrolidone, and 1 mM of phenylmethylsulfonyl fluoride, then centrifuged at 15,000× g for 20 min at 4 °C. Superoxide dismutase (SOD) activity was determined based on the capacity of the enzyme to inhibit the photoreduction of nitroblue tetrazolium (NBT) [27]. The supernatant was mixed with 63 μM NBT, 1.3 μM riboflavin, 13 mM methionine, 100 mM potassium phosphate buffer (pH 7.0). The reaction mixture kept at dark condition for 30 min and exposed to light condition for 20 min. One unit of SOD was defined as the amount of enzyme that inhibited the rate of NBT photoreduction by 50% at 560 nm. For measurement of ascorbate peroxidase (APOX) activity, 100 mM potassium phosphate buffer (pH 7.5), 0.2 mM H2O2, and 0.5 mM ascorbate were added to the enzyme extract. APOX activity was calculated by monitoring the decrease in absorbance at 290 nm for 1 min as AsA (coefficient, ε = 2.8 mM−1 cm−1) was oxidized [26]. Glutathione reductase (GR) activity was measured using the method used by Hasanuzzaman et al. [29]. The enzyme extract was reacted with 100 mM potassium phosphate buffer (pH 7.8), 1 mM EDTA, 0.2 mM NADPH, and 1 mM GSSG. The decrease in absorbance at 340 nm, as the NADPH (coefficient, ε = 6.2 mM−1 cm−1) was oxidized. For the measurement of glutathione peroxidase (GPOX) activity, 100 mM sodium phosphate buffer (pH 7.5), 2 mM GSH, 1 mM EDTA, 1 mM NaN3, 0.12 mM NADPH, 1 unit GR, and 0.6 mM H2O2 were added to the enzyme extract. The reaction was initiated with the addition of H2O2 and monitored the decrease in the NADPH absorbance at 340 nm for 1 min [29]. The activity was then calculated using an extinction coefficient of 6.62 mM−1 cm−1.

2.10. RNA Extraction and Quantitative Real-Time PCR Analysis

For total RNA isolation, fresh leaves (200 mg) were mixed with RNAiso Plus reagent (Takara, Nojihigashi 7-4-38 Kusatsu, Shiga, Japan), keep at room temperature for 5 min, and then centrifuged at 12,000× g for 5 min at 4 °C. The solution was separated into three layers, among them, the top liquid layer collected and mixed with isopropanol. After 10 min at room temperature, the mixed solution was centrifuged at 12,000× g for 10 min at 4 °C to precipitate the RNA. The pellet was washed with an equivalent amount of 75% ethanol, dried and dissolved with DEPC-treated water. Genomic DNA was digested with DNase I. First-strand complementary DNA (cDNA) was synthesized with a GoScript Reverse Transcription System (Takara). The qRT-PCR reactions were carried out on a BioRad CFX96 qPCR System using the TB Green Premix Ex Taq (Takara). Four biological replications were carried out for each treatment, each with two technical replicates. The relative expression levels were normalized to actin and calculated using the log2(2−ΔΔCT). Supplementary Table S1 provides the gene-specific primer used for qRT-PCR.

2.11. Statistical Analysis

The experiment was performed in a completely randomized design with four replicates per treatment. Duncan’s multiple range test was used to compare the means of separate replicates and the statistical significance was established at p < 0.05. All statistical measures were performed using SAS 9.1.3 (SAS Institute Inc., Cary, NC, USA).

3. Results

3.1. Leaf Water Potential, H2O2 Concentration and Antioxidant Enzyme Activities

Drought rapidly decreased leaf water potential (Ψw) up to −1.34 MPa after 4 days of drought stress, whereas no significant difference occurred in the control plants (Table 1). Drought caused H2O2 to accumulate from 4 days of the experiment, showing a 2.5-fold increase at day 14, compared to the control. However, the H2O2 concentration remained unchanged in the control plants throughout the experimental period (Table 1). Leaf biomass started to decrease after 4 days of drought treatment and then significantly decreased by 42.6% of control at day 14. No significant difference was observed between treatments in root biomass (Table 1).
Under drought conditions, SOD and GPOX activity increased considerably to ˃1.9-fold from days 4–10 and was then maintained at a similar level until day 14 (Figure 1A,D). In contrast, APOX and GR activity was markedly increased up to 3.1-fold during the initial 4 days and 2 days of drought stress, respectively, and then largely decreased but remained slightly higher than the control values during the later stage of the drought (days 10–14) (Figure 1B,C). No significant changes in antioxidant enzyme activities were observed in the control plants.

3.2. ABA and Sulfate Concentrations in Leaves, Roots, and Xylem

Endogenous ABA levels in leaves were significantly increased by drought stress, with a rapid increase of 3.6-fold at day 10 compared to the control (Figure 2A). Similarly, ABA concentrations in roots and xylem were gradually increased up to day 10 and were then maintained or slightly decreased in drought-stressed plants (Figure 2B,C). At day 14, the ABA concentration increased significantly in the phloem of drought-stressed plants (Supplementary Figure S1A). ABA concentration was not changed in the leaves, roots and xylem of control plants during the experimental period (Figure 2A–C). The sulfate concentration in the leaves of control plants markedly increased from days 4–14, whereas it showed the opposite trend in drought-stressed plants, resulting in a 50% of decrease compared to control (Figure 2D). Compared to the control plants, sulfate concentration in the roots and xylem of drought-stressed plants started to increase from day 4 and showed the largest increase (3.7 or 4.6-fold, respectively) at day 10 (Figure 2E,F). At day 14, sulfate concentration decreased markedly in the phloem of drought-stressed plants (Supplementary Figure S1B).

3.3. Cys and GSH Concentration, and the Expression of Sulfate Assimilation-Related Genes

There was no significant difference in Cys concentration between the control and drought-stressed plants during the early phase of the drought (days 0–4). Afterward, Cys concentration was greatly increased by 1.5- and 2-fold in leaves and roots of drought-stressed plants, respectively, compared to control plants (Figure 3A,C). GSH concentration in leaves gradually increased during the early phase of drought treatment and then significantly decreased by 37.7% of the initial level (Figure 3B). In roots, GSH concentration was largely increased after 4 days of drought stress and presented a 1.6-fold increase compared to the initial level (Figure 3D). No significant changes in GSH concentration were observed in the leaves and roots of control plants (Figure 3B,D). The expression of sulfate assimilation-related genes was observed in drought-stressed plants (Figure 4A). The expression of the adenosine-5-phosphosulfate reductase 2 (APR2) gene in drought-stressed plants was remarkably up-regulated to 2.2-fold in the first 2 days of drought stress, after which it continuously decreased to the control level (Figure 4A). Drought enhanced the expression of O-acetylserine(thiol)lyase (OASTL) and glutathione peroxidase (GPOX2) from day 4 onward and increased by 3.5- and 5.3-fold, respectively, at day 14 (Figure 4B,D). The expression of γ-glutamylcysteine synthetase 1 (GSH1) was rapidly up-regulated to 2.5-fold during the early phase of the drought, after which it decreased significantly to 60% of the initial level during the late stage (days 10–14) (Figure 4C). Similar to GSH1, the expression of glutathione reductase (GR1) was highly up-regulated only during the early stage (Figure 4E).

3.4. Redox Status under Drought Stress

The redox status in the leaves of control and drought-stressed plants is shown in Table 2 and the reduced GSH concentration remained the same, as shown in Figure 3B. Drought stress gradually increased GSSG concentration to 1.6- fold by day 14. The GSH/GSSG ratio increased slightly for the first 2 days of the drought treatment, after which it decreased significantly to <45.1% of the control during the late stage of the drought. During the 4 days of the early phase of the drought, NADPH concentration in the control plants remained unchanged, while it increased to 1.6-fold in drought-stressed plants; however, no significant difference was observed between control and drought-stressed plants during the late stage. NADP+ concentration in drought-stressed plants was highly increased to 1.6- and 1.9-fold at day 10 and day 14, respectively, compared to control plants. The ratio of NADPH/NADP+ increased up to day 4 and then rapidly decreased to 50% of the level in the control plants.

3.5. Correlation of Sulfate or ABA with Physiological Parameters Influenced by Drought Stress

The physiological relationship between sulfate or ABA, the identified Ψw and H2O2 concentrations and their scavenging enzymes, sulfate assimilation-related gene expression, and redox statuses, as affected by drought treatment, are presented in Table 3. Ψw was negatively correlated with sulfate and ABA concentration in the xylem, ABA, H2O2, GPOX, OASTL, and Cys, while being positively correlated with GR and redox status in the leaves of drought-stressed plants. Sulfate and ABA concentrations in the xylem were positively correlated with ABA, H2O2, GPOX, OASTL, and Cys, and were negatively correlated with sulfate, GR, GSH1, and redox status in leaves. Similar trends were observed in the correlation between ABA in leaves and other parameters, and the opposite trends were observed in correlation with sulfate in leaves.

4. Discussion

4.1. Drought Intensity-Responsive H2O2 Accumulation and Antioxidative Enzymatic Activity

The decrease in Ψw, caused by hydraulic stresses such as drought and salinity, has proven to be responsible for the decrease in stomatal conductance and the consequent reduction in photosynthetic CO2 assimilation [30,31], mineral uptake and assimilation [10,25,32] and the cell extension process [26]. In the present study, drought imposition over 14 days by reducing daily irrigation volume, decreased Ψw from −0.39 MPa to −1.34 MPa (Table 1). The Ψw at day 14 is higher than the range of −2.27 MPa to −2.33 MPa measured in white clovers exposed to 4 weeks of drought [26] or −2.0 MPa measured in drought-susceptible common bean cultivars [33], and lower than the range of −0.78 MPa to −0.9 MPa recorded in eight B. napus cultivars exposed to 7 days of water-deficit treatment [25]. In a previous study, we found that drought treatment for 14 days successfully induced drought stress in B. napus, as evidenced by the minimum Ψw value (−1.27 MPa), which resulted in the lowest photosynthetic activity accompanied with higher H2O2 accumulation and high lipid peroxidation levels [6]. In the present study, when the Ψw was ˃−0.57 MPa during the early phase of drought (days 0–4), H2O2 accumulation was not considerably changed (Table 1) with a strong activation of APOX (Figure 1B) and GR (Figure 1C), indicating that the ascorbate-glutathione pathway was highly induced during the early phase of drought stress. It is well established that APOX plays an active role in scavenging H2O2, particularly under mild stress [26,34]. Enhancement of GR activity was prominent at the early stress period under drought stress [35] and pathogen-infected conditions [36]. Therefore, during the early phase of drought, the strong activation of APOX and GR might be an important facet of drought acclimation that permits the preservation of membrane integrity. During the late phase of drought stress (days 10–14; Ψw ≤ −1.34 MPa), H2O2 accumulation was predominant (Table 1) and was accompanied with higher activation of SOD and GPOX activity (Figure 1C,F). Higher enhancement of SOD enzyme activity suggested that under oxidative stress, more H2O2 was needed to trigger the production of ROS by the electron transport chain; similar results were observed in B. napus exposed to 15 days of drought [27]. The activation of SOD at the late phase during the decrease in APOX and GR activity (Figure 1A–C) indicates that cell oxidation occurred. In addition, GPOX activity after 10 days of drought treatment (Ψw ≤ −1.34 MPa) enhanced to approximately 4-fold compared to control plants (Ψw ≥ −0.54 MPa) (Figure 1D). Similarly, overexpression of GPOX increased the rate of GSH generation and oxidation [37]. These results indicate that higher GPOX activation during the late drought phase is a factor for the cell-oxidizing process of reduced GSH to its disulfide form (GSSG) [38].

4.2. Drought Intensity-Responsive Changes in Sulfate, ABA Allocation, and S-Assimilates in Leaves

Drought generally decreases the mineral uptake kinetics per unit root, which might slow down nutrient uptake [39] or decrease the expression of nutrient-uptake proteins in roots [32]. In the present study, during the early 4 days of drought treatment, sulfate concentrations did not change markedly in either leaves or roots (Figure 2D,E), and the increase in GSH was significant only at day 4; however, during the late phase of drought stress (i.e., days 10–14; Ψw ≤ −1.34 MPa), sulfate concentration in leaves decreased by approximately 50% (Figure 2D), accompanied with accumulation of Cys (Figure 3A) and a loss of GSH (Figure 3B) when compared to the control. A significant decrease in GSH in leaves during the late phase might be due to insufficient sulfate supply [15] and to the limiting role of glutathione synthetase [40]. Several points should be highlighted here: the abundance of sulfate in roots and in xylem sap (Figure 2E,F), and the Cys accumulation in both leaves and roots (Figure 3A,C) even though there was a significant decrease in the GSH pool in leaves, indicate that the availability of sulfate and/or Cys in leaves is not the exclusive determinant for the GSH system in leaves, which is possibly linked to other regulatory components. In fact, among the literature previously published, stress-responsive Cys and GSH concentrations have not been consistent, as the two major sulfate assimilates were affected by stress intensity, sulfur allocation into different organs and nutritional state [15,41,42].
It has been widely established that stress-induced ROS (especially H2O2) activates phytohormone signaling, and vice versa with their possible interactive regulatory functions [6,27,43,44]. Among these interactions, ABA-dependent signaling pathway has been studied in greater detail in different plants and stressors. For instance, H2O2-stimulated-ABA accumulation has shown to be a critical response to severe drought symptom development [6]. As expected, endogenous ABA levels began to increase in both leaves and roots from day 4 of drought stress, to a larger extent during the late phase (days 10–14; Ψw ≤ −1.34 MPa) (Figure 2A,B), when H2O2 accumulation concurrently occurred (Table 1). Drought-induced H2O2 and ABA accumulation during the late phase was concomitant with a prominent increase in sulfate concentration in roots and in xylem sap but not in leaves (Figure 2D–F). Similarly, in Arabidopsis, sulfate application increased H2O2 levels in guard cells to a similar extent as the ABA level [20] by specific activation of plasma membrane-localized NADPH oxidases in an ABA-dependent manner [6,20]. In maize (Zea mays L.), sulfate was the sole ion that increased in xylem sap following a concomitant increase in xylem-borne ABA transport during 12 days of withholding water [18], leading to ABA-dependent stomatal closure [20,22]. Our previous studies have clearly shown that drought-responsive H2O2 accumulation with progressing drought stress intensity leads to an activation of ABA synthesis and its signaling [6,45,46]. Therefore, the enhanced ABA level is mainly due to H2O2-mediated activation of oxidative burst signaling (OXI1) and mitogen-activated protein kinases (MAPKs) [47], rather than sulfate alone (e.g., the decreased sulfate level in leaves). The enhanced ABA level and its signaling in tune activate H2O2 production leading to drought symptom development [6,45,46]. Consistent with the previous studies above mentioned, drought-enhanced ABA and sulfate in xylem during the late phase (Figure 2C,F) resulted in an increase in Cys (Figure 3A) and a decrease in GSH concentration in leaves (Figure 3B). These data strongly suggest that xylem-borne sulfate and/or ABA, which were enhanced especially during late stage of drought, might suppress the Cys incorporation into GSH leading to a loss of the GSH pool.

4.3. Sulfate and/or ABA Roles in Regulating Sulfate Assimilation

To further assess the regulatory roles of sulfate and/or ABA in the sulfate assimilatory pathway, the expression of genes involved in sulfate assimilation was measured in leaves exposed to drought. The expression of APR2 was markedly enhanced only for the early 4 days, while suppressed during the late stage (days 10–14) in the leaves exposed to drought (Figure 4A). Consistently, in Arabidopsis, ABA did not affect the mRNA levels of APR isoforms and the regulation of APR was not changed in mutants deficient in ABA accumulation (aba1 and aba2) or ABA signaling (abi1 and abi2) [48]. It thus suggests that APR regulation during the late phase of drought is clearly ABA-independent, and that APR2 has to be rapidly activated to allow Cys synthesis to meet the increased GSH level in the early drought phase (Figure 3A,B). In contrast, the OASTL expression was hardly activated in the early 4 days and then highly enhanced during the late stage of drought stress (Figure 4B). Barroso et al. [41] reported the salt-induced OASTL in an ABA-dependent manner and the external ABA-driven activation of OASTL. Therefore, APR2 and OASTL act differently in regulating the drought-responsive sulfate assimilatory pathway: APR is involved in Cys synthesis as an acclamatory response in an ABA-independent manner, while OASTL is at the late stage of drought stress (Figure 4A,B). This study has shown a drought-responsive suppression of GSH1 expression in the leaves at a late stage (days 10–14) (Figure 4C). Several results have shown that sulfate and/or Cys affect ABA synthesis and the endogenous level of ABA [18,19,20], and sulfate acts as a mobile signal stimulating Cys synthesis to trigger ABA synthesis and signaling [18,49]. The present data and those from past literature strongly suggest that during the late phase of drought-driven xylem, sulfate activates ABA synthesis and signaling in leaves and consequently leads to an ABA-mediated suppression of the GSH synthesis gene GSH1 (Figure 4C), resulting in a decrease in GSH concentration.

4.4. Interactions between Sulfate and ABA in GSH-Based Redox Control

In the context of of an interactive function between sulfur and ABA in the stress-responsive biological action, especially in stomatal movement [18,19,20,49], we assessed the sulfate- and/or ABA-mediated GSH-based redox control. During the early phase of drought treatment (day 0–4), the resulting GSH/GSSG redox state transiently shifted toward a slightly reduced state on the initial 2 days. This transient increase in GSH (Figure 3B) and GSH/GSSG ratio at day 2 (Table 2) might be attributed to a strong activation of ROS scavenging enzymes in the ascorbate-glutathione cycle (APOX and GR; Figure 1B,C), as well as an enhanced expression of GSH1 (Figure 4C), as an early acclimation reaction as shown by Tausz et al. [50]. During the late phase of drought stress (days 10–14, Ψw ≤ −1.34 MPa), enzymatic activity of GR and expression of GR1 were remarkably suppressed (Figure 1C and Figure 4E) in a concurrent increase in ABA (Figure 2A). Thus, the decreased GSH/GSSG ratio at this late phase (Table 2) would be attributed to ABA-mediated suppression of GR, which allows the recycling of GSSG back to GSH, using NADPH as the reducing power [51]. In contrast, GPOX activity and GPOX2 gene expression were greatly increased during the late phase of drought stress (Figure 1D and Figure 4D). Furthermore, the activation of GPOX activity to drought intensity was nearly parallel to the increased ABA level in leaves and xylem sap (Figure 2A,C; Table 3), suggesting the ABA-mediated regulation of GPOX activity. In a genome-wide analysis of the GPOX gene family in B. napus, ABA-responsive enhancement of BnGPOX1 under salinity and PEG-induced water stress conditions was characterized [52]. Therefore, during the late phase of drought (Ψw ≤ −1.34 MPa), ABA-activated GPOX, with an antagonistic repression of GR, would be responsible for shifting GSH- and NADPH-based redox to more oxidative state along with enhanced H2O2 accumulation, consistent with a general concept of eco-physiological stress responses [50]. The present data clearly indicate that the loss of reducing potential in the GSH- and NADPH-based redox system, as a clear indicant of drought-induced oxidation process, might be attributed to the decrease in GSH synthesis and further oxidation of GSH catalyzed by GPOX with an antagonistic suppression of GR in a sulfate-activated ABA-dependent manner.

5. Conclusions

A time-course analysis in relation to drought intensity clearly showed that drought-responsive changes in sulfate and ABA allocation in different organs would be an important stress response, which further coordinates the regulation of the sulfate assimilatory pathway toward GSH metabolism and the GSH redox control. Regression analysis revealed that the decrease in Ψw with progression drought stress was closely correlated with the increase in sulfate and ABA level in xylem and leaves each other (Table 3). The physiological responses to drought intensity were distinguished by two distinct phases characterized by (1) a transient increase in GSH pool and in GSH/GSSG ratio with a strong activation of the H2O2 scavenging enzymes in the ascorbate-glutathione cycle (APOX and GR) for the early phase (days 0–4, Ψw ≥ −0.54 MPa) and (2) a decrease in GSH with Cys accumulation resulting in a remarked loss of reducing potential in both GSH- and NADPH-based redox system, accompanied by a remarked GPOX activation with an antagonistic suppression of GR in a sulfate-activated ABA-dependent manner during the late phase (days 10–14; Ψw ≤ −1.34 MPa) (Figure 5). To the best of our knowledge, the present findings are the first report of drought intensity-induced changes in sulfate and ABA coordinates in the regulation of sulfate assimilation toward GSH metabolism and GSH-based redox. Nevertheless, a critical point “sulfate-dependent de novo synthesis of ABA, as well as ABA-mediated redox control by ABA itself or by oxidative stress signal” needs to be well-defined.

Supplementary Materials

The following supporting information can be downloaded at: https://www.mdpi.com/article/10.3390/metabo12121190/s1. Supplementary Table S1. Specific primers used for qRT-PCR. Supplementary Figure S1. Changes in concentration of ABA (A) and sulfate (B) in phloem of well-watered (control) or drought-stressed plant at day 14. Data represented as means ± S.E. for n = 4. Asterisks indicate a significant difference compared to the control (water application): * p < 0.05, *** p < 0.001.

Author Contributions

B.-R.L. and T.-H.K.: conceptualization, methodology, investigation, and writing original draft. B.-R.L., S.-H.P., V.H.L. and D.-W.B.: formal analysis. B.-R.L., S.-H.P., V.H.L., D.-W.B. and T.-H.K.: review and editing. T.-H.K.: supervision, project administration, and funding acquisition. All authors have read and agreed to the published version of the manuscript.

Funding

This work was supported by a grant from the National Research Foundation of South Korea under project NRF-2021R1A4A1031220.

Institutional Review Board Statement

Not applicable.

Informed Consent Statement

Not applicable.

Data Availability Statement

Data is contained within the article and its Supplementary Materials.

Conflicts of Interest

The authors declare no conflict of interest.

References

  1. Gilbert, S.M.; Clarkson, D.T.; Cambridge, M.; Lambers, H.; Hawkesford, M.J. SO42– deprivation has an early effect on the content of ribulose-1,5-biphosphate carboxylase/oxygenase and photosynthesis in young leaves of wheat. Plant Physiol. 1997, 115, 1231–1239. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  2. Lee, B.R.; Muneer, S.; Jung, W.J.; Avice, J.C.; Ourry, A.; Kim, T.H. Partitioning of newly absorbed and previously stored nitrogen and sulphur under sulphate deficient nutrition. J. Plant Nutr. 2014, 37, 1702–1716. [Google Scholar] [CrossRef]
  3. Muneer, S.; Lee, B.R.; Kim, K.Y.; Park, S.H.; Zhang, Q.; Kim, T.H. Involvement of sulphur nutrition in modulating iron deficiency responses in photosynthetic organelles of oilseed rape (Brassica napus L.). Photosynth. Res. 2014, 119, 319–329. [Google Scholar] [CrossRef] [PubMed]
  4. Lee, B.R.; Zaman, R.; Avice, J.C.; Ourry, A.; Kim, T.H. Sulfur use efficiency is a significant determinant of drought stress tolerance in relation to photosynthetic activity in Brassica napus cultivars. Front. Plant Sci. 2016, 7, 459. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  5. Foyer, C.H.; Noctor, G. Redox signaling in plants. Antioxid. Redox Signal. 2013, 18, 2087–2090. [Google Scholar] [CrossRef]
  6. Park, S.H.; Lee, B.R.; La, V.H.; Mamun, M.A.; Bae, D.W.; Kim, T.H. Characterization of salicylic acid- and abscisic acid-mediated photosynthesis, Ca2+ and H2O2 accumulation in two distinct phases of drought stress intensity in Brassica napus. Environ. Exp. Bot. 2021, 186, 104434. [Google Scholar] [CrossRef]
  7. Baxter, A.; Mittler, R.; Suzuki, N. ROS as key players in plant stress signaling. J. Exp. Bot. 2014, 65, 1229–1240. [Google Scholar] [CrossRef]
  8. Choudhury, F.K.; Rivero, R.M.; Blumwald, E.; Mittler, R. Reactive oxygen species, abiotic stress and stress combination. Plant J. 2017, 90, 856–867. [Google Scholar] [CrossRef]
  9. Mittler, R. Oxidative stress, antioxidants and stress tolerance. Trends Plant Sci. 2002, 7, 405410. [Google Scholar] [CrossRef]
  10. Lee, B.R.; Jin, Y.L.; Avice, J.C.; Cliquet, J.B.; Ourry, A.; Kim, T.H. Increased proline loading to phloem and its effects on nitrogen uptake and assimilation in water-stressed white clover (Trifolium repens). New Phytol. 2009, 182, 654–663. [Google Scholar] [CrossRef]
  11. Khan, N.A.; Anjum, N.A.; Nazar, R.; Iqbal, N. Increased activity of ATP sulfurylase and increased contents of cysteine and glutathione reduce high cadmium-induced oxidative stress in mustard cultivar with high photosynthetic potential. Russ. J. Plant Physiol. 2009, 56, 670–677. [Google Scholar] [CrossRef]
  12. Szalai, G.; Kellős, T.; Galiba, G.; Kocsy, G. Glutathione as an antioxidant and regulatory molecule in plants under abiotic stress conditions. J. Plant Growth Regul. 2009, 28, 66–80. [Google Scholar] [CrossRef]
  13. Meyer, A.J. The integration of glutathione homeostasis and redox signaling. J. Plant Physiol. 2008, 165, 1390–1403. [Google Scholar] [CrossRef]
  14. Foyer, C.H.; Noctor, G. Ascorbate and glutathione: The heart of the redox hub. Plant Physiol. 2011, 155, 2–18. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  15. Ahmad, N.; Malagoli, M.; Wirtz, M.; Hell, R. Drought stress in maize causes differential acclimation responses of glutathione and sulfur metabolism in leaves and roots. BMC Plant Biol. 2016, 16, 247. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  16. Astolfi, S.; Zuchi, S. Adequate S supply protects barley plants from adverse effects of salinity stress by increasing thiol contents. Acta Physiol. Plant. 2013, 35, 175–181. [Google Scholar] [CrossRef]
  17. Aoyama, K.; Nakaki, T. Glutathione in Cellular Redox Homeostasis: Association with the Excitatory Amino Acid Carrier 1 (EAAC1). Molecules 2015, 20, 8742–8758. [Google Scholar] [CrossRef] [Green Version]
  18. Ernst, L.; Goodger, J.Q.D.; Alvarez, S.; Marsh, E.L.; Berla, B.; Lockhart, E.; Jung, J.; Li, P.; Bohnert, H.J.; Schachtman, D.P. Sulphate as a xylem-born chemical signal precedes the expression of ABA biosynthetic genes in maize roots. J. Exp. Bot. 2010, 61, 3395–3405. [Google Scholar] [CrossRef] [Green Version]
  19. Cao, M.J.; Wang, Z.; Zhao, Q.; Mao, J.L.; Speiser, A.; Wirtz, M.; Hell, R.; Zhu, J.K.; Xinag, C.B. Sulfate availability affect ABA levels and germination response to ABA and salt stress in Arabidopsis thaliana. Plant J. 2014, 77, 604–615. [Google Scholar] [CrossRef]
  20. Batool, S.; Uslu, V.V.; Rajab, H.; Ahmad, N.; Waadt, R.; Geiger, D.; Malagoli, M.; Xiang, C.B.; Hedrich, R.; Rennenberg, H.; et al. Sulfate is incorporated into cysteine to trigger ABA production and stomatal closure. Plant Cell 2018, 30, 2973–2987. [Google Scholar] [CrossRef]
  21. Sierla, M.; Waszczak, C.; Vahisalu, T.; Kangasjarvi, J. Reactive oxygen species in the regulation of stomatal movements. Plant Physiol. 2016, 170, 1569–1580. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  22. Malcheska, F.; Ahmad, A.; Batool, S.; Muller, H.M.; Ludwig-Muller, J.; Kreuzwieser, J.; Randewig, D.; Hänsch, R.; Mendel, R.R.; Hell, R.; et al. Drought enhanced xylem sap sulfate closes stomata by affecting ALMT12 and guard cell ABA synthesis. Plant Physiol. 2017, 174, 798–814. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  23. Okuma, E.; Jahan, M.S.; Munemasa, S.; Hossain, M.A.; Muroyama, D.; Islam, M.M.; Ogawa, K.; Watanabe-Sugimoto, M.; Nakamura, Y.; Shimoishi, Y.; et al. Negative regulation of abscisic acid-induced stomatal closure by glutathione in Arabidopsis. J. Plant Physiol. 2011, 168, 2048–2055. [Google Scholar] [CrossRef] [PubMed]
  24. Speiser, A.; Silbermann, M.; Dong, Y.; Haberland, S.; Uslu, V.V.; Wang, S.; Banagsh, S.A.K.; Reichelt, M.; Meyer, A.J.; Wirtz, M.; et al. Sulfur partitioning between glutathione and protein synthesis determines plant growth. Plant Physiol. 2018, 177, 927–937. [Google Scholar] [CrossRef] [Green Version]
  25. Lee, B.R.; Jin, Y.L.; Park, S.H.; Zaman, R.; Zhang, Q.; Avice, J.C.; Ourry, A.; Kim, T.H. Genotypic variation in N uptake and assimilation estimated by 15N tracing in water deficit-stressed Brassica napus. Environ. Exp. Bot. 2015, 109, 73–79. [Google Scholar] [CrossRef]
  26. Lee, B.R.; Kim, K.Y.; Jung, W.J.; Avice, J.C.; Ourry, A.; Kim, T.H. Peroxidases and lignification in relation to the intensity of water-deficit stress in white clover (Trifolium repens L.). J. Exp. Bot. 2007, 58, 1271–1279. [Google Scholar] [CrossRef] [Green Version]
  27. La, V.H.; Lee, B.R.; Islam, M.T.; Park, S.H.; Jung, H.I.; Bae, D.W.; Kim, T.H. Characterization of salicylic acid-mediated modulation of the drought stress responses: Reactive oxygen species, proline, and redox state in Brassica napus. Environ. Exp. Bot. 2019, 157, 1–10. [Google Scholar] [CrossRef]
  28. Gaitonde, M. A spectrophotometric method for the direct determination of cysteine in the presence of other naturally occurring amino acids. Biochem. J. 1967, 104, 627–633. [Google Scholar] [CrossRef] [Green Version]
  29. Hasanuzzaman, M.; Hossain, M.A.; Fujita, M. Nitric oxide modulates antioxidant defense and the methylglyoxal detoxification system and reduces salinity-induced damage of wheat seedlings. Plant Biotecnol. Rep. 2011, 5, 353–365. [Google Scholar] [CrossRef]
  30. Lee, B.R.; Jin, Y.L.; Jung, W.J.; Avice, J.C.; Bertrand, A.M.; Ourry, A.; Park, C.W.; Kim, T.H. Water-deficit accumulates sugars by starch degradation—Not by de novo synthesis—In white clover leaves (Trifolium repens L.). Physiol. Plant. 2008, 134, 403–411. [Google Scholar] [CrossRef]
  31. Pinheiro, C.; Chaves, M.M. Photosynthesis and drought: Can we make metabolic connections from available data? J. Exp. Bot. 2011, 62, 869–882. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  32. Bista, D.R.; Heckathorn, S.A.; Jayawardena, D.A.; Mishra, S.; Boldt, J.K. Effects of drought on nutrient uptake and the levels of nutrient-uptake proteins in roots of drought-sensitive and -tolerant grasses. Plants 2018, 7, 28. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  33. Cruz de Carvalho, M.H.; Contour-Anse, D. (h)GR, beans and drought stress. Plant Signal. Behav. 2008, 3, 834–835. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  34. Foyer, C.H.; Noctor, G. Redox sensing and signalling associated with reactive oxygen in chloroplasts, peroxisomes and mitochondria. Physiol. Plant. 2003, 119, 355–364. [Google Scholar] [CrossRef] [Green Version]
  35. Liu, J.; Wang, X.; Hu, Y.; Hu, W.; Bi, Y. Glucose-6-phosphate dehydrogenase plays a pivotal role in tolerance to drought stress in soybean roots. Plant Cell Rep. 2013, 32, 415–429. [Google Scholar] [CrossRef]
  36. Fortunato, A.A.; Debona, D.; Bernardeli, A.M.A.; Rodrigues, F.A. Changes in the antioxidant system in soybean leaves infected by Corynespora cassiicola. Phytopathology 2015, 105, 1050–1058. [Google Scholar] [CrossRef] [Green Version]
  37. Zhang, L.; Wu, M.; Teng, Y.; Jia, S.; Yu, D.; Wei, T.; Chen, C.; Song, W. Overexpression of the glutathione peroxidase 5 (RcGPOX5) gene from Rhodiola crenulata increases drought tolerance in Salvia miltiorrhiza. Front. Plant Sci. 2019, 9, 1950. [Google Scholar] [CrossRef]
  38. Mittova, V.; Theodoulou, F.L.; Kiddle, G.; Gómez, L.; Volokita, M.; Tal, M.; Foyer, C.H.; Guy, M. Coordinate induction of glutathione biosynthesis and glutathione-metabolizing enzymes is correlated with salt tolerance in tomato. FEBS Lett. 2003, 554, 417–421. [Google Scholar] [CrossRef] [Green Version]
  39. Rouphael, Y.; Cardarelli, M.; Schwarz, D.; Franken, P.; Colla, G. Effects of drought on nutrient uptake and assimilation in vegetable crops. In Plant Responses to Drought Stress, 1st ed.; Aroca, R., Ed.; Springer: Berlin, Germany, 2012; pp. 171–195. [Google Scholar]
  40. Herrera, K.; Cahoon, R.E.; Kumaran, S.; Jez, J. Reaction mechanism of glutathione synthetase from Arabidopsis thaliana: Site-directed mutagenesis of active site residues. J. Biol. Chem. 2007, 282, 17157–17165. [Google Scholar] [CrossRef] [Green Version]
  41. Barroso, C.; Romero, L.C.; Cejudo, F.J.; Vega, J.M.; Gotor, C. Salt-specific regulation of the cytosolic O-acetylserine(thiol)lyase gene from Arabidopsis thaliana is dependent on abscisic acid. Plant Mol. Biol. 1999, 40, 729–736. [Google Scholar] [CrossRef]
  42. Kocsy, G.; Szalai, G.; Galiba, G. Effect of osmotic stress on glutathione and hydroxymethyl-glutathione accumulation in wheat. J. Plant Physiol. 2004, 161, 785–794. [Google Scholar] [CrossRef] [PubMed]
  43. Xia, X.J.; Zhou, Y.H.; Shi, K.; Zhou, J.; Foyer, C.H.; Yu, J.Q. Interplay between reactive oxygen species and hormones in the control of plant development and stress tolerance. J. Exp. Bot. 2015, 66, 2839–2856. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  44. Hieno, A.; Naznin, H.A.; Inaba-Hasegawa, K.; Yokogawa, T.; Hayami, N.; Nomoto, M.; Tada, Y.; Yokogawa, T.; Higuchi-Takeuchi, M.; Hanada, K.; et al. Transcriptome analysis and identification of a transcriptional regulatory network in the response to H2O2. Plant Physiol. 2019, 180, 1629–1646. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  45. La, V.H.; Lee, B.R.; Islam, M.T.; Park, S.H.; Lee, H.; Bae, D.W.; Kim, T.H. Antagonistic shifting from abscisic acid- to salicylic acid-mediated sucrose accumulation contributes to drought tolerance in Brassica napus. Enviorn. Exp. Bot. 2019, 162, 38–47. [Google Scholar] [CrossRef]
  46. Lee, B.R.; La, V.H.; Park, S.H.; Mamun, M.A.; Bae, D.W.; Kim, T.H. H2O2-responsive hormonal status involves oxidative burst signaling and proline metabolism in Rapeseed leaves. Antioxidants 2022, 11, 566. [Google Scholar] [CrossRef]
  47. Rentel, M.C.; Lecourieux, D.; Ouaked, F.; Usher, S.L.; Petersen, L.; Okamoto, H.; Knight, H.; Peck, S.C.; Grierson, C.S.; Hirt, H.; et al. OXI1 kinase is necessary for oxidative burst-mediated signaling in Arabidopsis. Nature 2004, 427, 858–861. [Google Scholar] [CrossRef]
  48. Koprivova, A.; North, K.A.; Kopriva, S. Complex signaling network in regulation of adenosine 5’-phosphosulfate reductase by salt stress in Arabidopsis roots. Plant Physiol. 2008, 146, 1408–1420. [Google Scholar] [CrossRef] [Green Version]
  49. Rajab, H.; Khan, M.S.; Malagoli, M.; Hell, R.; Wirtz, M. Sulfate-induced stomata closure requires the canonical ABA signal transduction machinery. Plants 2019, 8, 21. [Google Scholar] [CrossRef] [Green Version]
  50. Tausz, M.; Sircelj, H.; Grill, D. The glutathione system as a stress marker in plant ecophysiology: Is a stress–response concept valid? J. Expt. Bot. 2004, 55, 1955–1962. [Google Scholar] [CrossRef]
  51. Marty, L.; Siala, W.; Schwarzlander, M.; Fricker, M.D.; Wirtz, M.; Sweetlove, L.J.; Meyer, Y.; Meyer, A.J.; Reichheld, J.P.; Hell, R. The NADPH-dependent thioredoxin system constitutes a functional backup for cytosolic glutathione reductase in Arabidopsis. Proc. Natl. Acad. Sci. USA 2009, 106, 9109–9114. [Google Scholar] [CrossRef]
  52. Li, W.; Huai, Z.; Li, P.; Raza, A.; Mubarik, M.S.; Habib, M.; Fiaz, S.; Zhang, B.; Pan, J.; Khan, R.S.A. Genome-wide characterization of glutathione peroxidase (GPX) gene family in rapeseed (Brassica napus L.) revealed their role in multiple abiotic stress response and hormone signaling. Antioxidants 2021, 10, 1481. [Google Scholar] [CrossRef] [PubMed]
Metabolites 12 01190 g001 550
Figure 1. Changes in activities of superoxide dismutase (SOD, (A)), ascorbate peroxidase (APOX, (B)), glutathione reductase (GR, (C)) and glutathione peroxidase (GPOX, (D)) in the leaves of well-watered (control) or drought-stressed plants for 14 days. The black and red lines indicate control and drought stress, respectively. Data are represented as means ± S.E. for n = 4. Asterisks indicate a significant difference between well-watered and drought-stressed plants: * p < 0.05, ** p < 0.01, *** p < 0.001.
Figure 1. Changes in activities of superoxide dismutase (SOD, (A)), ascorbate peroxidase (APOX, (B)), glutathione reductase (GR, (C)) and glutathione peroxidase (GPOX, (D)) in the leaves of well-watered (control) or drought-stressed plants for 14 days. The black and red lines indicate control and drought stress, respectively. Data are represented as means ± S.E. for n = 4. Asterisks indicate a significant difference between well-watered and drought-stressed plants: * p < 0.05, ** p < 0.01, *** p < 0.001.
Metabolites 12 01190 g001
Metabolites 12 01190 g002 550
Figure 2. Changes in the concentration of ABA (A–C) and sulfate (D–F) in leaves (A,D), roots (B,E), and xylem (C,F) of well-watered (control) or drought-stressed plants for 14 days. The black and red lines indicate control and drought stress, respectively. Data represented as means ± S.E. for n = 4. Asterisks indicate a significant difference between well-watered and drought-stressed plants: * p < 0.05, ** p < 0.01, *** p < 0.001.
Figure 2. Changes in the concentration of ABA (A–C) and sulfate (D–F) in leaves (A,D), roots (B,E), and xylem (C,F) of well-watered (control) or drought-stressed plants for 14 days. The black and red lines indicate control and drought stress, respectively. Data represented as means ± S.E. for n = 4. Asterisks indicate a significant difference between well-watered and drought-stressed plants: * p < 0.05, ** p < 0.01, *** p < 0.001.
Metabolites 12 01190 g002
Metabolites 12 01190 g003 550
Figure 3. Changes in concentration of cysteine (A,C) and glutathione (B,D) in leaves (A,B) and roots (C,D) in well-watered (control) or drought-stressed plants for 14 days. The black and red lines indicate control and drought stress, respectively. Data are represented as means ± S.E. for n = 4. Asterisks indicate a significant difference between well-watered and drought-stressed plants: * p < 0.05, ** p < 0.01, *** p < 0.001.
Figure 3. Changes in concentration of cysteine (A,C) and glutathione (B,D) in leaves (A,B) and roots (C,D) in well-watered (control) or drought-stressed plants for 14 days. The black and red lines indicate control and drought stress, respectively. Data are represented as means ± S.E. for n = 4. Asterisks indicate a significant difference between well-watered and drought-stressed plants: * p < 0.05, ** p < 0.01, *** p < 0.001.
Metabolites 12 01190 g003
Metabolites 12 01190 g004 550
Figure 4. Relative expression of sulfate assimilation-related genes, adenosine-5-phosphosulfate reductase 2 (APR2, (A)), O-acetylserine(thiol)lyase (OASTL, (B)), γ-glutamylcysteine synthetase 1 (GSH1, (C)), glutathione peroxidase (GPOX2, (D)) and glutathione reductase (GR1, (E)) in leaves of drought-stressed plants for 14 days. The values in drought-stressed plants at day 0 were set to 1. Data are represented as means ± S.E. for n = 4. The different letters indicate values that ate significantly difference at p < 0.05 according to Duncan’s multiple range test.
Figure 4. Relative expression of sulfate assimilation-related genes, adenosine-5-phosphosulfate reductase 2 (APR2, (A)), O-acetylserine(thiol)lyase (OASTL, (B)), γ-glutamylcysteine synthetase 1 (GSH1, (C)), glutathione peroxidase (GPOX2, (D)) and glutathione reductase (GR1, (E)) in leaves of drought-stressed plants for 14 days. The values in drought-stressed plants at day 0 were set to 1. Data are represented as means ± S.E. for n = 4. The different letters indicate values that ate significantly difference at p < 0.05 according to Duncan’s multiple range test.
Metabolites 12 01190 g004
Metabolites 12 01190 g005 550
Figure 5. Schematic diagram for the proposed interactive regulation of sulfate to ABA-mediated regulation of sulfur assimilation and GSH redox in two distinct phase of drought intensity. Changes in metabolites, enzyme activities, and gene expressions in related to ROS scavenging, ABA, sulfur assimilation and GSH-based redox status are indicated by black, red, and blue letters, respectively. The circle size indicates the amount of metabolites. The thickness of the arrow indicates the strength of induced or depressed response.
Figure 5. Schematic diagram for the proposed interactive regulation of sulfate to ABA-mediated regulation of sulfur assimilation and GSH redox in two distinct phase of drought intensity. Changes in metabolites, enzyme activities, and gene expressions in related to ROS scavenging, ABA, sulfur assimilation and GSH-based redox status are indicated by black, red, and blue letters, respectively. The circle size indicates the amount of metabolites. The thickness of the arrow indicates the strength of induced or depressed response.
Metabolites 12 01190 g005
Table
Table 1. Changes in the leaf water potential, H2O2 concentration, leaf and root biomass in the well-watered (control) or drought-stressed plants for 14 days.
Table 1. Changes in the leaf water potential, H2O2 concentration, leaf and root biomass in the well-watered (control) or drought-stressed plants for 14 days.
Physiological ParametersDays after Treatment
/Treatment0241014
Leaf water potential (Ψw, MPa)
Control−0.39−0.42−0.45−0.54−0.53
Drought−0.39−0.49−0.57 *−1.12 **−1.34 ***
H2O2 concentration (nmol g−1 FW)
Control2.973.063.163.083.47
Drought2.973.543.857.86 ***8.67 ***
Leaf biomass (Dry matter, g plant−1)
Control8.238.5610.8914.0716.48
Drought8.238.478.92 **9.49 ***9.46 ***
Root biomass (Dry matter, g plant−1)
Control5.865.096.287.148.16
Drought5.865.356.056.647.23
Data represented as means ± S.E. for n = 4. Asterisks indicate significant difference between well-watered and drought-stressed plants at each harvest day: * p < 0.05, ** p < 0.01, *** p < 0.001.
Table
Table 2. Changes in GSH- and NADPH-based redox status in the leaves of Brassica napus 14 days after drought imposition.
Table 2. Changes in GSH- and NADPH-based redox status in the leaves of Brassica napus 14 days after drought imposition.
GSHGSSGGSH/GSSGNADPHNADP+NADPH/NADP+
DayTreatment(nmol g−1 FW)(nmol g−1 FW)Ratio(nmol g−1 FW)(nmol g−1 FW)Ratio
0Control582 ± 3544.3 ± 3.713.2 ± 0.73.2 ± 0.36.0 ± 0.40.53 ± 0.04
Drought582 ± 3544.3 ± 3.713.2 ± 0.73.2 ± 0.36.0 ± 0.40.53 ± 0.04
2Control560 ± 4645.5 ± 5.712.4 ± 0.63.7 ± 0.37.1 ± 0.60.53 ± 0.04
Drought697 ± 37 *50.4 ± 4.313.9 ± 0.5 *5.0 ± 0.4 *6.9 ± 0.50.73 ± 0.09 *
4Control620 ± 5848.1 ± 4.612.9 ± 0.83.3 ± 0.46.5 ± 0.40.51 ± 0.07
Drought741 ± 42 *63.3 ± 5.2 *11.7 ± 0.44.9 ± 0.3 **7.3 ± 0.40.67 ± 0.07
10Control575 ± 3051.2 ± 4.811.3 ± 0.53.6 ± 0.45.6 ± 0.50.65 ± 0.11
Drought392 ± 28 **78.2 ± 5.9 **5.1 ± 0.7 ***3.0 ± 0.49.2 ± 0.8 **0.33 ± 0.02 **
14Control606 ± 4851.8 ± 4.911.7 ± 0.73.9 ± 0.35.4 ± 0.30.73 ± 0.08
Drought363 ± 33 **81.4 ± 6.2 **4.5 ± 0.6 ***3.8 ± 0.310.3 ± 0.7 ***0.37 ± 0.04 **
Data are represented as means ± S.E. for n = 4. Asterisks indicate significant difference between well-watered and drought-stressed plants at each harvest day: * p < 0.05, ** p < 0.01, *** p < 0.001.
Table
Table 3. Linear correlations of sulfate and ABA with the descriptive parameters of H2O2 production and scavenging, sulfur assimilation and redox status as affected by drought stress for 14 days.
Table 3. Linear correlations of sulfate and ABA with the descriptive parameters of H2O2 production and scavenging, sulfur assimilation and redox status as affected by drought stress for 14 days.
XylemLeaves
ΨwSulfateABASulfateABAH2O2GRGPOXOASTLGSH1CysGSHGSH/
GSSG		NADPHNADPH/
NADP+
Ψw-0.922 ***−0.915 ***0.866 ***−0.972 ***−0.965 ***0.372−0.966 ***−0.974 ***0.616 **−0.830 ***0.845 ***0.958 ***0.3580.789 ***
Sulfate in xylem--0.963 ***−0.847 ***0.978 ***0.959 ***−0.4050.975 ***0.949 ***−0.607 **0.86 3 ***−0.880 ***−0.974 ***−0.467 *−0.826 ***
ABA in xylem---−0.821 ***0.945 ***0.929 ***−0.2340.955 ***0.934 ***−0.461 *0.855 ***−0.771 ***−0.952 ***−0.349−0.765 ***
Sulfate in leaves----−0.837 ***−0.874 ***0.509 *−0.857 ***−0.898 ***0.538 *−0.694 ***0.769 ***0.864 ***0.3580.708 ***
ABA in leaves-----0.971 ***−0.3890.983 ***0.960 ***−0.635 **0.868 ***−0.887 ***−0.976 ***−0.426−0.816 ***
Ψw, leaf water potential. The values measured in the drought stressed plants were used for correlation analysis. Correlation coefficient (r) and significant level of difference are reported; n = 15. * p < 0.05, ** p < 0.01, *** p < 0.001.
Publisher’s Note: MDPI stays neutral with regard to jurisdictional claims in published maps and institutional affiliations.

Share and Cite

MDPI and ACS Style

Lee, B.-R.; Park, S.-H.; La, V.H.; Bae, D.-W.; Kim, T.-H. Drought-Induced Xylem Sulfate Activates the ABA-Mediated Regulation of Sulfate Assimilation and Glutathione Redox in Brassica napus Leaves. Metabolites 2022, 12, 1190. https://doi.org/10.3390/metabo12121190

AMA Style

Lee B-R, Park S-H, La VH, Bae D-W, Kim T-H. Drought-Induced Xylem Sulfate Activates the ABA-Mediated Regulation of Sulfate Assimilation and Glutathione Redox in Brassica napus Leaves. Metabolites. 2022; 12(12):1190. https://doi.org/10.3390/metabo12121190

Chicago/Turabian Style

Lee, Bok-Rye, Sang-Hyun Park, Van Hien La, Dong-Won Bae, and Tae-Hwan Kim. 2022. "Drought-Induced Xylem Sulfate Activates the ABA-Mediated Regulation of Sulfate Assimilation and Glutathione Redox in Brassica napus Leaves" Metabolites 12, no. 12: 1190. https://doi.org/10.3390/metabo12121190

Note that from the first issue of 2016, this journal uses article numbers instead of page numbers. See further details here.

Article Metrics

Back to TopTop