ORIGINAL RESEARCH article
Soil Selenium (Se) Biofortification Changes the Physiological, Biochemical and Epigenetic Responses to Water Stress in Zea mays L. by Inducing a Higher Drought Tolerance
- 1Department of Agricultural, Food and Environmental Sciences, University of Perugia, Perugia, Italy
- 2Department for Sustainable Food Process, Catholic University of the Sacred Heart, Piacenza, Italy
Requiring water and minerals to grow and to develop its organs, Maize (Zea mays L.) production and distribution is highly rainfall-dependent. Current global climatic changes reveal irregular rainfall patterns and this could represent for maize a stressing condition resulting in yield and productivity loss around the world. It is well known that low water availability leads the plant to adopt a number of metabolic alterations to overcome stress or reduce its effects. In this regard, selenium (Se), a trace element, can help reduce water damage caused by the overproduction of reactive oxygen species (ROS). Here we report the effects of exogenous Se supply on physiological and biochemical processes that may influence yield and quality of maize under drought stress conditions. Plants were grown in soil fertilized by adding 150 mg of Se (sodium selenite). We verified the effects of drought stress and Se treatment. Selenium biofortification proved more beneficial for maize plants when supplied at higher Se concentrations. The increase in proline, K concentrations and nitrogen metabolism in aerial parts of plants grown in Se-rich substrates, seems to prove that Se-biofortification increased plant resistance to water shortage conditions. Moreover, the increase of SeMeSeCys and SeCys2 forms in roots and aerial parts of Se-treated plants suggest resistance strategies to Se similar to those existing in Se-hyperaccumulator species. In addition, epigenetic changes in DNA methylation due to water stress and Se treatment were also investigated using methylation sensitive amplified polymorphism (MSAP). Results suggest that Se may be an activator of particular classes of genes that are involved in tolerance to abiotic stresses. In particular, PSY (phytoene synthase) gene, essential for maintaining leaf carotenoid contents, SDH (sorbitol dehydrogenase), whose activity regulates the level of important osmolytes during drought stress and ADH (alcohol dehydrogenase), whose activity plays a central role in biochemical adaptation to environmental stress. In conclusion, Se-biofortification could help maize plants to cope with drought stress conditions, by inducing a higher drought tolerance.
The use of water in agriculture is unevenly spread with a peak in summer when water is least available, maximizing detrimental impacts (Sharpe, 2009). More than 90% of agricultural area in the EU is rain fed, so crop water stress often underlies the inter-annual variability observed in grain production (EUROSTAT, 2010).
Maize (Zea mays L.) is one of the most important food crops in the world (it is produced on nearly 100 million hectares) and, along with rice and wheat, provides at least 30% of food calories to more than 4.5 billion people in 94 countries. It is one of the most important cereals both for human and animal consumption. Furthermore, maize is an important candidate crop for ethanol production. Maize is a major summer crop in the irrigated areas of the Mediterranean region. It is a water demanding crop that can reach high grain yields (10–12 t ha-1) only when water and nutrients are not limited (Pandey et al., 2000; Çakir, 2004). Water demand for maize is concentrated in the summer months when availability is lowest. Access to an adequate water supply, including more efficient use of all available water, is therefore critical to achieving improved yields.
Drought stress is one of the major environmental factors that inhibits many metabolic processes and consecutively slows down the development of the plant with loss of yield and productivity around the world. The arid and semi-arid regions of the globe, especially in developing countries, are at great risk because they are facing acute shortage of water.
Plants respond to environmental stress by alteration of the pattern of protein synthesis. These stress-induced proteins are considered to enhance the plants’ ability to survive the conditions of stress. The limited or non-availability of water reduces growth of crop plants through the effects on various physiological and biochemical processes.
Selenium had long been considered to be a toxic element for higher organisms, but in Schwarz and Foltz (1957) reported that low concentrations of Se are essential for dietary intake and interchangeable with vitamin E. Later it was discovered that Se mitigating environmental stress protects the cells of rats against intracellular oxidative damage (Rotruck et al., 1973). Since then, owing to its physiological and toxicological importance, Se has become an element of interest which has been investigated in humans, animals and in plants.
Selenium toxicity (400 μg kg-1) in humans and animals causes disruption of the digestive and nervous systems but, on the other hand, deficiency leads to free radical damage, such as greater risk of tumour formation, hypertension and atherosclerosis. Cereals are the major source of Se among plants (50–60 μg kg-1). Se content of food is highly dependent on soil Se bioavailability and the ability of plants to take up and accumulate Se in edible tissues (Bañuelos et al., 2017). In the soil, selenite is less bioavailable to plants than selenate, because the former is preferentially absorbed by iron oxides and/or hydroxides. Owing to this behavior in the soil, selenite is preferable to selenate; it is not dispersed with rainwater or irrigation, thus also minimizing the risks of pollution of the groundwater (Zhu et al., 2009).
Selenium is not considered essential for plant growth, but recent studies indicate its physiological and anti-oxidant properties play beneficial roles in plants exposed to various abiotic stress (Cartes et al., 2010). Se improves plant tolerance to DS by regulating water status (Yao et al., 2009), increasing chlorophyll in plant leaves (Dong et al., 2013), protecting against cadmium toxicity (Elkahoui et al., 2004), reducing damage caused by UV-radiation oxidative stress (Valkama et al., 2003) and enhancing chlorophyll content under light stress (Seppänen et al., 2003).
Selenium may also protect plants from fungal infection and invertebrate phloem-feeders (Hanson et al., 2004). Moreover, it has also been reported to improve the yield of food crops like wheat (Broadley et al., 2010), barley (Ducsay et al., 2009), rice (Wang et al., 2013), and maize (Chilimba et al., 2012).
Abiotic stresses such as low and high temperature (Akladious, 2012; Balal et al., 2016), salinity (Abul-Soud and Abd-Elrahman, 2016), heavy metals (Li et al., 2016), excess water and drought (Nawaz et al., 2015) could be regulated by exogenous Se, associated with the increased activity of GPX and antioxidants activity with a simultaneous decrease in lipid peroxidase activity. In Proietti et al. (2013), the effects of Se on plant growth under DS stimulate the activity of the antioxidant enzymes CAT and SOD, which were depressed in response to drought.
For example, an increase in antioxidant enzyme activity after Cd treatment has been detected in the roots and leaves of Phaseolus vulgaris L. (Chaoui et al., 1997) and Raphanus sativus L. (Vitória et al., 2001), such as the accumulation of H2O2, causing oxidative stress in these plants. DNA methylation play important roles in the establishment of developmental programs in fungi, plants and animals. (Teyssier et al., 2008). Environmental stimuli, such as heavy metals, water and salt stress, are known to alter cytosine methylation throughout the genome and specific loci (Lukens and Zhan, 2007). Plants use epigenetic regulatory strategies, such as DNA methylation, to maintain genomic plasticity, allowing relatively rapid adaptation to new conditions without changing the DNA sequence (Causevic et al., 2005). Generally, hypermethylation is correlated with gene silencing, while hypomethylation is connected with active transcription (Paszkowski and Whitham, 2001). Moreover, some authors suggest a role played by selenium in preventing DNA methylation changes and in reducing the amount of ROS, that, in turn, are believed to be the trigger of methylation status changes (Filek et al., 2008; Peng and Zhang, 2009). Therefore, in this paper, the possible involvement of epigenetic changes in maize in response to DS and/or Se supplementation was investigated through MSAP. This technique has been applied in several species to detect the methylation status and is based on the use of two isoschizomers, HpaII and MspI, recognizing 5′-CCGG-3′ sequences but have differential sensitivity to cytosine methylation status.
The aims of the work were: (i) to confirm the effectivity of the Se-biofortification technique used, which was able to transfer Se from soil to roots and aerial parts; (ii) to verify if Se-biofortification can increase the drought tolerance of maize plants and which mechanisms would be involved in this water stress tolerance, studying specifically the role of pigments, proteins, ions and DNA methylation.
Materials and Methods
Type of Soil Used
A clay-loam soil was air-dried, passed through a 2 mm sieve and analyzed for its basic physical and chemical properties. Water-holding capacity was 300 mL kg-1 and the permanent wilting point was 120 mL kg-1. On a dry weight basis: a pH (H2O) of 8.3, CaCO3 concentration of 240 g kg-1, total organic C of 9.9 g kg-1, total N concentration of 1.0 g kg-1, CSC of 20.1 cmol(+) kg-1 and total Se concentration of 12.0 mg kg-1. Soil analyses were performed following official methods (Carter and Gregorich, 2007). For the determination of Se concentration, acid digestion of soil [0.25 g was performed with a mixture of HNO3 and H2O2 (8:2, v/v)]. The determination of the Se in digested materials was accomplished by using an atomic absorption spectrophotometer (US Environmental Protection Agency [EPA], 1996), equipped with a graphite furnace and a deuterium lamp (Shimadzu AA-6800, GF-AAS, “Shimadzu Corp.”, Tokyo, Japan). The back-ground correction was carried out using a matrix modifier of Pd(NO3)2 in 0.5 M in HNO3 (Sigma-Aldrich, St. Louis, MO, United States).
Soil spiking was performed by taking samples of the same air dried and sieved (<2 mm) soil. The soil (3 kg) in the Se treated samples has been fertilized by adding 150 mg of Se (328 mg of sodium selenite) to each pot before sowing. The Se salt was added to the soil and then stirred for 4 h.
The bioassay was carried out at the greenhouse of the Department of Agricultural, Food and Environmental Sciences, University of Perugia (Central Italy, 12°23-E, 43°5-N), in May 2015, with minimum temperature ranging between 10°C and 15°C and maximum temperature ranging from 20°C to 36°C.
The experimental design was completely randomized with four treatment factors: normal irrigation without Se treatment (WW-Se), DS without Se treatment (DS-Se), normal irrigation with Se treatment (WW+Se) and Se under DS condition (DS+Se) and six replicates, for a total of 24 pots. Maize (cv Fidias) was sown (11 May 2015) in 0.20 m diameter PVC pots filled with 3,000 g of air-dried soil, using three seeds per pot. For the samples under normal irrigation, the pots were sub-irrigated every 2nd day to recover water-holding capacity. For the stressed samples, DS was imposed on 5 June 2015, on plants 0.25 m high. From this date, irrigations were suspended to let the soil reach a water content equal to 25% of the available water. Later, the pots were sub irrigated every 2nd day to recover a water content equal to 25% of the available moisture content. The amount of water needed to reach 100 and 25%, respectively, of available moisture content in the soil were determined by considering the average weight of the pots and giving the same amount of water to all pots in the same irrigation treatment. Once in a week the sub-irrigations were performed by using a solution of fertilizer for hydroponics (FLORY 9, Agrochimica, Italy), containing 5% total N, 7% P2O5, 22% K2O, 6% MgO and less than 10 μg Se kg-1. Maize plants were grown up until pot size represented an obstacle to normal development; in detail, they were harvested at 0.50 m height (14 July 2015). After harvesting, all plants were rinsed quickly in deionized water, weighed and split into the different organs: roots and aerial parts (aerial parts and leaves).
Plant aerial part height was determined by placing samples on black chart paper with a 1 m ruler alongside them. Portions of roots and aerial parts harvested were weighed and immediately used for the analysis that required fresh material (Se speciation and proline). Aerial part dry weight was obtained by drying samples in a forced-draft oven at 60°C for 48 h and ground to pass through a 0.5-mm sieve. Other portions were collected and rapidly frozen at -80°C and used for DNA extraction (MSAP technique).
Total Chlorophylls and Carotenoids
The concentration of chlorophylls (Chlorophyll a, ChlA; Chlorophyll b, ChlB) and carotenoids (Car) were determined only in the fresh aerial part sample following the method of Lichtenthaler and Wellburn (1983).
The sum of ChlA and ChlB was reported as the total concentration of chlorophylls (TotChl). Results were then expressed as milligrams per gram of fresh weight (mg g-1 FW).
Determination of Total Se Concentration
Dry vegetable samples (0.25 g) with additions of 8 mL of concentrated HNO3 (65% v/v; Carlo Erba, Milan, Italy) and 2 mL of H2O2 (30% v/v, Carlo Erba) were microwave digested (ETHOS One high-performance microwave digestion system; Milestone Inc., Sorisole, Bergamo, Italy) (Cubadda et al., 2010). The digested solutions were filtered using a 0.22 μm filter after appropriate dilution with Milli-Water (18.2 MΩ), according to US Environmental Protection Agency [EPA] (1996), and the concentration of total Se was determined by ICP-MS (Agilent 7900, Agilent Technologies, United States) with Octopole Reaction System (ORS system). The standard solutions of Se were used by diluting the corresponding stock solutions (Se standard 1000 mg L-1 for AAS TraceCert Sigma-Aldrich 89498). This method was accurately validated with a recovery test (n = 3) by adding from a Se standard solution (4 mg L-1) into the mixture of Se-enriched sample and nitric acid prior to digestion.
Analysis of Se Species in Leaves and Roots
Approximately 1 g of fresh leaves and roots were accurately weighed and chopped with 10 mL of solution 2.0 mg mL-1 of protease (Protease Type XIV, Sigma-Aldrich P5147 -1 g). An ultrasound probe was used and sonication time was 3 min. All of the samples were stirred in a water bath at 37°C for 3 h. After the extraction, the samples were allowed to cool to room temperature and centrifuged for 10 min at 9,000 rpm. The supernatant was filtered through 0.22 μm Millex GV filters (Millipore Corporation, Billerica, MA, United States).
The Se standards (Na2SeO3, Na2SeO4, selenomethionine (SeMet), selenocystine (SeCys2), selenium methylselenocysteine (SeMeSeCys) were obtained from Sigma (St. Louis, MO, United States) and prepared in ultrapure (>18 MΩ) water.
Speciation of Se was performed by HPLC-ICP-MS (HPLC 1100 coupled with ICP-MS 7700x, both Agilent Technologies, United States) on an anion exchange column (Hamilton, PRP-X100, 250 × 4.6 mm, 5 μm particle size). The mobile phase was made using ammonium acetate (Carlo Erba, Milan, Italy) with gradient elution. Detailed information is summarized in Supplementary Table S1. The samples were analyzed at different dilutions and selenocompounds were identified in extracts by retention time matching with the standard substances spiked in the sample extracts.
Limit of detection (LODs = 3σ), expressed as μg L-1, were 0.9, 0.7, 0.3, 0.6, and 0.2 for SeCys2, MeSeCys, SeMet, Se(IV) and Se(VI), respectively.
The concentration of proline was estimated in all plants by HPLC with a method described by Palmerini et al. (2006). The HPLC used was a Jasco 880-PU (Jasco, Tokyo, Japan) equipped with a fluorimetric detector Jascho 821-FP. The proline was measured on leaves (2 g of leaves) homogenized in 10 mL of ultrapure H2O with an ultra turrax T25 (Tanke and Kunkel Ika Labortechnik, Staufen, Germany) for 3 min on ice. The homogenates were then centrifuged at 5,000 × g for 10 min and an aliquot of the supernatant (1 mL) of the extract was deproteinized with 0.200 mL HClO4 (20% v/v) in ice and centrifuged at 8,000 rpm 5 min. At the supernatant were added 0.200 mL of KOH (20% by weight) and the precipitate of KClO4 was removed by centrifugation at 8,000 for 5 min. An aliquot of the supernatant (0.050 mL) was mixed with 0.150 mL (0.4 M) borate pH 9 with 0.050 mL of o-ftaldeide chloride (150 mM) (OPA) in methanol, and 0.1 mL of 7-chloro-4 -nitrobenzo 2 bone-1,3-diazole (25 mM) (NBD-Cl) in methanol. The reaction performed at 60°C for 3 min was interrupted in ice with 0.100 mL HCl (1 M). The derivatized (0.020 mL) of each sample was injected into a RP-18 Lichrosor column, (15 cm × 4.6 mm ID) of the HPLC and eluted in instrumentation under isocratic conditions with H2O/CH3CN (93:7) used as mobile phase. The solvents used were previously passed on a 0.22 μm filter (Millipore Corporation, Billerica, MA, United States). The NBD-derivatives were determined to ex470 nm e em 530 nm. The NBD- proline was eluted in 6.5 min and quantified with a standard solution of proline. Proline (0.043 M) and hydroxy-proline (0.038 M), used as internal standard, were diluted 1–100 in H2O and then 0.050 mL derivatized as the samples (0.01 mL) analyzed by HPLC. The results were expressed for proline as nmol g-1 TF.
Ionic Concentrations in Aerial Parts
Ionic concentrations in plant extracts was determined by ion chromatography with conductivity detection (Portlab Hplc System Stayer, Milan, Italy). The method used was described for the determination of the ionic concentration of vegetable samples by ion chromatography with suppressed conductivity detection (Cataldi et al., 2003). Leaf tissues, approximately 0.25 g of (-Se) and (+Se) plants were homogenized in 5 mL of pure water; the suspension was shaken for 20 min and then centrifuged at 3,000 rpm for 12 min. Prior to the injection, the extracts were filtered through single-use 0.22 μm nylon filters to remove any particulate matter. The extracts obtained at room temperature yielded chromatographic profiles with substantial differences in the relative concentrations of F-, Cl-, Br-, NO3-, PO43-, and SO42- as well as of Na+, K+. The results stated in this paper represent the mean of three repetitions performed for each sample. The concentrations of anions were both calculated as g 100 g-1, while for cations as mg g-1.
Determination of Total Nitrogen (Kjeldahl Method)
Two grams of dry sample were digested in a Kjeldahl digestion flask, as in the official method used for the determination of total nitrogen in plant tissue (Isaac and Johnson, 1976) and which led to the use of the calculation N × 6.25 to convert nitrogen concentration into protein concentration (Nprot). Determinations were made on all reagents alone (blank determinations).
DNA Extraction and MSAP Technique
For MSAP analysis, total genomic DNA, extracted from maize leaves, collected at 60 DAS using the DNeasy Plant Mini Kit (Qiagen, Milan, Italy), following the protocol reported in Marconi et al. (2013) and Bocchini et al. (2015). The 12 primer combinations used for the selective amplifications are reported in Supplementary Table S2. The differential sensitivity of HpaII and MspI to methylation allows the separation of the amplified fragments into four types. Type I is given by bands present in both enzyme combinations (EcoRI/HpaII and EcoRI/MspI). Type II correspond to bands present only in EcoRI/HpaII, indicating the hemimethylated state of DNA, i.e., the result of the methylation in one strand but not in its complementary strand. Type III bands appeared only in EcoRI/MspI, representing the case of full CG methylation (internal cytosine) whereas type IV, is the case of full methylation at both cytosines, and represents the absence of bands in both enzyme combinations.
Bioassay data relating to the concentrations of the different forms of Se in maize roots and aerial parts were submitted to two-way ANOVA, by considering water-stress and Se-biofortification as factors, with two levels each. The ‘water-stress × Se-biofortification’ interaction was always significant and the means for the four combinations were compared using Fisher’s LSD at P = 0.05. In order to summarize the results, principal component analysis (PCA) was used on the two-way matrix with treatments along the rows and all the observed variables along the columns [concentrations in sodium (Na) potassium (K), proteic nitrogen (Nprot), chlorophyll A (ChlA), chlorophyll B (ChlB), total chlorophyll (TotChl), carotenoids (Car), nitrates (Nitr), fluorides (Fluo), sulphates (Sulph), phosphates (Phosph) and chlorides (Chlor)]. Data were standardized prior to analysis and results were displayed in a distance-biplot (Legendre and Legendre, 2012).
In MSAP analysis, to determine the significance of the sources of variation, the recorded data (bands) were processed by analysis of variance (ANOVA). First, for each Type of methylation status (Types I, II, III, and IV), several one factor completely randomized ANOVAs were performed considering the stress treatments (i.e., WW+Se vs. WW-Se; WW+Se vs. DS+Se; WW+Se vs. DS-Se; WW-Se vs. DS+Se; WW-Se vs. DS-Se and DS+Se vs. DS-Se) as the experimental factor. The same simple one factor ANOVA was also carried out for the total methylated bands (i.e., the sum of bands of Types II, III, and IV), the full methylated bands (i.e., the sum of Types III and IV) and hemi methylated bands (Type II).
Secondly, a two-factor ANOVA with 6 replicates was performed, by considering Stress and Class (Total, Full and Hemi Methylated bands) as factors. In addition, the significance of effects was tested by using F tests. Pairwise comparisons were tested for the stress × class combinations. Finally, the mean ± standard deviation (SD) derived from six biological replicates per experiment was calculated for each MSAP band type.
Silver Staining and DNA Sequences of Water-Selenium-Related Fragments
Some samples, which were chosen on the basis of interesting polymorphisms, were run on acrylamide gels and silver stained with the aim of isolating and sequencing the selected bands as reported in Marconi et al. (2013). Interesting polymorphic bands were then excised from gels and rehydrated with 100 μL of milli-Q water o/n at 4°C. Tubes were centrifuged at maximum speed for 5 min and the supernatant transferred into a fresh tube. Aliquots of 5 μL were used as a template for re-amplification by PCR in a 25 μL reaction volume. All PCR reactions were carried out with the same Eco and MpsI/HpaII primer combination used in selective amplification step with this profile: 94°C for 1 min, 30 cycles of denaturation at 94°C for 1 min, annealing at 55°C for 1 min, extension at 72°C for 1 min and ending with a 20 min extension step at 72°C.
One microliter of the re-amplified DNA was cloned into pCR4-TOPO vector using the TOPO TA cloning kit for sequencing (Invitrogen, Carlsbad, CA, United States). Three plasmids for each transformation were purified from 5 mL of o/n culture of E. coli, in LB medium, using the GenElute Plasmid miniprep kit (Sigma-Aldrich, Milan, Italy). The sequences of both strands were determined after running sequencing reactions, obtained with BigDye® Terminator v3.1 Cycle Sequencing Kit, (Applied Biosystems, Foster City, CA, United States) on an ABI 3130xl Genetic Analyzer (Applied Biosystems, Foster City, CA, United States). Sequences identified through MSAP were used as queries in NCBI Release 2151, Uniprot release 2016_082 (The UniProt Consortium, 2017) and MaizeGDB3 by using B73 RefGen_v3 websites.
Effects of Se-Biofortification on Plant Morphological, Chemical and Biochemical Parameters
In untreated (-Se) plants, DS significantly reduced aerial part weight by 37% (Table 1 and Supplementary Table S3). Regarding Se-biofortified (+Se) plants, DS significantly reduced aerial part weight by 24% (Table 1 and Supplementary Table S3). Therefore, although DS caused a reduction in maize development, the treatment with Se was able to reduce these adverse effects by at least 13%. Regarding irrigated plants (WW), Se-biofortification significantly increased the aerial part weight by 32% (Table 1 and Supplementary Table S3). In terms of drought stressed (DS) plants, Se biofortification significantly increased the aerial part weight by 59%. Therefore, the beneficial effect of Se-treatment was higher on plants in water stressed conditions, resulting in an increase of the development of the treated plants by at least 27%, compared to the untreated controls (Table 1 and Supplementary Table S3).
TABLE 1. Weight and total, inorganic [Se(IV)+Se(VI)] and organic (Total Se-Inorganic Se) Se concentrations in maize aerial parts and roots.
Significant differences in total Se concentration were observed in aerial parts and roots of (+Se) and (-Se) maize plants, regardless of the stress conditions (Table 1). As concerns roots, Se bio-fortification enhanced the total Se concentrations by 5.1 and 5.2 times in irrigated and in drought stressed plants, respectively. Regarding aerial parts, Se bio-fortification enhanced total Se concentrations by 3.9 and 3.5 times in irrigated and in drought stressed plants, respectively. In the aerial part, the above increase in total Se appeared to be mainly due to the Se organic forms which increased by about ten times (Table 1) in (+Se) plants. On the contrary, in (+Se) plants the inorganic Se concentrations are similar to those of (-Se) plants. As concerns roots, the increase in total Se concentrations seems to be due both to inorganic and organic Se forms.
Considering the ‘aerial part/root’ ratios in relation to total Se concentration, Se-treated plants showed a decrease, both in irrigated and in drought stressed plants (Table 2).
TABLE 2. Ratio between Se in aerial parts and roots (DW), for total Se, organic Se (total Se less inorganic Se) and inorganic Se [sum Se(VI) and Se(IV)].
Selenium bio-fortification of irrigated plants caused significant increases of SeCys2 (448%), SeMeSeCys (698%), SeMet (383%), Se(IV) (449%), and Se(VI) (326%) in the roots, with respect to (-Se) (Table 3). Likewise, Se bio-fortification of drought stressed plants caused significant increases of SeCys2 (273%), SeMeSeCys (225%), and Se(VI) (379%) (Table 3). Regarding aerial parts, Se bio-fortification of irrigated plants caused significant increases of SeCys2, SeMeSeCys of 88.7 and 40.9% and significant decrease of SeMet of 29.5%. Likewise, in drought stressed plants, Se bio-fortification caused significant increases of SeCys2 (68.4%) and SeMeSeCys (34.8%), while SeMet significantly decreased (-36.4%). It is interesting to note that in irrigated plants, the Se organic forms which increased most with Se bio-fortification were SeMeSeCys and SeCys2, both in roots and in aerial parts; however, in drought stressed plants, Se bio-fortification mostly increased SeCys2, both in roots and in aerial parts (Table 3). As concerns Se inorganic forms, in irrigated plants, Se(IV) increased more than Se(VI) both in roots and in aerial parts; otherwise, in roots of S plants, Se(VI) was the form which increased the most. Concerning aerial parts, Se(IV) and Se(VI) showed similar increases (Table 3).
The production of proline in the aerial part of (+Se) plants, both irrigated and drought stressed, increased significantly compared to that of the (-Se) plants (Figure 1). Moreover, DS imposed on the (-Se) plants did not produce any increase in proline, confirming that this increase was due to Se (Figure 1).
FIGURE 1. Proline (Pro) concentrations in aerial parts. WW, well watered; DS, drought stress. (WW–Se) normal irrigation without Se treatment, (DS–Se) drought stress without Se treatment, (WW+Se) normal irrigation with Se treatment and (DS+Se) Se under drought stress conditions. Data for each experiment were compared separately using Fisher’s LSD test (P < 0.05). Different letters indicate significant differences between treatments.
The whole set of results relating to maize aerial part samples was summarized by using a PCA (Figure 2 and Supplementary Table S4) and the model thus obtained explains 86% of the total variance of data with two principal components (69 and 17%, respectively). The resulting biplot shows that the concentrations of Chlorophyll A (ChlA), chlorophyll B (ChlB), Total chlorophyll (TotChl), carotenoids (Car), nitrates (Nitr), fluorides (Fluo), sulphates (Sulph), phosphates (Phosph), and chlorides (Chlor) are mainly related to the positioning of observations along the first component (x-axis), while proteic nitrogen (Nprot), sodium (Na), and potassium (K) are mainly related to the positioning along the second component (y-axis). In this respect, DS-Se lies on the first quadrant (positive scores for both PCs) and it shows small values on all the observed components; WW-Se lies on the second quadrant (negative score for PC1 and positive for PC2) and was high in Chlorophyll A, B, carotenoids and nitrates and relatively low in all other compounds. WW+Se lies on the third quadrant (negative scores for both PCs) and shows high values of all compounds, while DS+Se lies on the fourth quadrant and it was low in all compounds, except Na, K, and Nprot. Indeed, water stress moves the observation along the x-axis and thus determines a decrease in all compounds except K, Na, and Nprot, which tend to increase in DS+Se plants. On the other hand, the treatment with Se moves the observations along the y-axis and treated plants tend to recover their concentrations in Na, K, and Nprot (irrigated and drought stressed) and in fluorides, sulfates, phosphates and chlorides (only irrigated plants).
FIGURE 2. PCA on correlation matrix for the concentration of several compounds in aerial parts (DW). Sodium (Na); potassium (K); proteic nitrogen (Nprot); chlorophyll A (ChlA); chlorophyll B (ChlB); Total chlorophyll (TotChl); carotenoids (Car); nitrates (Nitr); fluorides (Fluo); sulphates (Sulph); phosphates (Phosph) and chlorides (Chlor); (WW–Se) normal irrigation without selenium treatment, (DS–Se) drought stress without Se treatment, (WW+Se) normal irrigation with Se treatment and (DS+Se) Se under drought stress conditions.
Extent and Pattern of DNA Methylation Under Control Conditions and Drought Stress/Selenium Treatment
A total of 653 clear and reproducible bands were amplified from 12 primer combinations (Supplementary Table S2) in plants grown either under normal irrigation or DS. Under control conditions (WW-Se), the total methylation of CCGG sites averaged 61.2%; this value decreased (-0.35% corresponding to 60.85%) in the presence of selenium (+Se), with the same irrigation conditions (Supplementary Table S5). In drought stressed samples (DS), DNA methylation level in the presence of Se was lower than in -Se samples (60.77% vs. 60.57%).
Effect of Drought Stress and Presence of Se on the Level of Methylation in Maize
The 653 amplification products were classified as shown in Table 4. Patterns A–C represents monomorphic classes in which methylation pattern is the same following either the WW-Se or the WW+Se/ DS-Se/ DS+Se samples. Patterns D–H are indicative of cytosine demethylation, whereas possible cytosine methylation events induced in WW+Se/ DS-Se/ DS+Se are represented by patterns NO. Selenium treatment in normal irrigation (WW+Se) samples was found to induce 7 demethylation events and 5 methylation events. On the contrary, DS induced 8 and 3 methylation and 6 and 5 demethylation events in the absence (DS-Se) or presence (DS+Se) of Se treatment, respectively.
TABLE 4. Variations in DNA methylation pattern of Z. mays in different grown conditions: normal irrigation without (WW-Se) or with (WW+Se) selenium treatment and drought stress without (DS-Se) or with (DS+Se) selenium treatment.
Drought stress effect was significant (P < 0.05) for Non-, Total-, Full-Methylated bands (Tables 5A–C) and accounted for 28.7, 28.7, and 40.4% of the total sum of squares (SS), respectively, when WW-Se were compared with DS-Se and with DS+Se plants. Also, for the comparison between the same stresses and considering the comparison between Total- vs. Full- and Total- vs. Hemi- Methylated bands (Tables 5D,E), the stress effect was significant and accounted for 0.18 and 0.01% of total SS, respectively. However, the main source of variation for Total- vs. Full- Methylated and Total- vs. Hemi- Methylated bands was the effect Class (Tables 5D,E), that accounted for 99.6 and 99.9% of the total SS relative to main effects (Stress+Class+Rep). For Class Hemi-Methylated, the Types (i.e., I, II, III, and IV), the all possible comparison between Types and the other comparison between Classes (i.e., Full- vs. Hemi Methylated) only the effect Class was significant (data not shown).
TABLE 5. Analysis of variance for each different status of methylation (Not-, Total-, Full-, and Hemi- methylated bands) and for each pairwise combination of them considering all the pairwise combinations of stresses (drought stress and Se treatment).
Sequencing and Bioinformatics Analysis of Methylated DNA Fragments
Nine differentially methylated DNA bands were excised from acrylamide gels, cloned and sequenced. The resulting sequences were blasted against the databases at NCBI, Uniprot and MaizeGDB websites. The sequences of three fragments were too short (under 75 nt) and other three resulted in no similarities. Three sequences showed a significant match (E-value lower that 0.001) and were significantly associated with Z. mays genes: (i) ZM_1 sequence (size 112 bp, accession number MG949279) showed a significant similarity (94.12% identity, E-value: 8.845e-7) with a maize gene encoding for chloroplast PSY1 (accession number Q6SMR0); (ii) ZM_2 sequence (size 174 bp, accession number MG949280) displayed was very like (96.43% identity, E-value: 6.776e-5) with a maize gene encoding for SDH (accession number DQ191049); (iii) ZM_3 sequence (size 106 bp, accession number MG949281) showed high similarity (97.37% identity, E-value 3.463e-11) with a maize gene encoding for an ADH1 (accession number AY691949).
The results gathered in this study show the effectiveness of Se bio-fortification in increasing water stress tolerance in maize by limiting the reduction of plant biomass due to water shortage conditions, as also reported by Nawaz et al. (2016). Hartikainen et al. (2000) reported that Se effects on plants depend on its concentration. At lower rates, Se stimulated growth of ryegrass seedlings in pot experiments, while at high doses it acted as pro-oxidant reducing yields and induced metabolic disturbances. This was also confirmed by Hawrylak-Nowak et al. (2015) in cucumber where root and aerial part biomass was inversely related to Se concentration.
Moreover, other studies showed that the exogenous application of Se increased the tolerance of plants to drought-induced oxidative damage by enhancing their antioxidant defense systems (Hasanuzzaman and Fujita, 2011; Proietti et al., 2013).
Regarding the effectiveness of the Se-biofortification method used in this study, the percentage increase of total Se concentration in the irrigated (WW) and drought stressed (DS) plants was of the same magnitude.
Our results show that Se bio-fortification (+Se) determined an increase in the Se amount in roots, which was greater than that observed in aerial parts (Table 1). Such behavior should be attributed to the selection of selenite as a fortifying agent, because of its greater persistence in the soil compared to selenate (Wang et al., 2013) and with little translocation properties to aerial parts (Arvy, 1993; De Souza et al., 1998; Zayed et al., 1998; Hopper and Parker, 1999; Terry et al., 2000; Ximénez-Embún et al., 2004; Li et al., 2008; Liu and Gu, 2009). As reported by Zhu et al. (2009), translocation of Se from roots to aerial parts depends on which Se species is supplied to the plant. In plants fed with selenate, Se is readily translocated to the aerial part. By contrast, in selenite-treated plants, most of Se stays in the roots and it is rapidly converted to organic forms; most of it, however, remains in inorganic and water-insoluble forms, as confirmed by our results (Table 2).
Data obtained from Se-speciation highlighted how the maize plant’s capacity to tolerate large tissue Se concentrations is primarily related to the ability to divert Se away from the accumulation of SeCys and SeMet, which might be incorporated into non-functional proteins through the synthesis of less toxic Se metabolites. Pilon-Smits and Quinn (2010) indicated that toxic SeCys can be methylated to form SeMeSeCys, a non-toxic free amino acid, by SeCys methyltransferase (SMT). Because, in contrast to Se-Cys and Se-Met, SeMeSeCys does not enter proteins and it can be safely accumulated to high levels in plant tissues, which in part explains the high tolerance of hyperaccumulators to Se. Furthermore, Zhang et al. (2006) reported, in Arabidopsis thaliana L., that tolerance to both selenate and selenite has been correlated with high SeCys2 concentrations.
These findings suggest resistance strategies to Se similar to those existing in Se hyperaccumulator species. Moreover, as SeMeSeCys is the form of Se which confers the best anticarcinogenic properties, this is advantageous from a human nutrition perspective (Wang et al., 2013).
The maize plants grown in Se-rich soils produced more proline than those grown in the untreated ones, regardless of water stress conditions. When exposed to stress factors, plants react by accumulating metabolites, such as amino acids, and proline is one of them. Several reports indicate that stressful environments may result in an overproduction of proline in the plants, which may contribute to stress tolerance, by maintaining cell turgor or osmotic balance, stabilizing membranes and thereby preventing electrolyte leakage; this brings concentrations of ROS within normal ranges, thus preventing oxidative burst in plants (Hayat et al., 2012). A similar increase of proline production has been reported by Khan et al. (2015), which studied the influence of Se in the protection of photosynthetic capacity of wheat (Triticum aestivum) against cadmium stress; they reported that an application of Se in the growth substrate of wheat seeds alleviated Cd-induced oxidative stress by increasing proline accumulation as a result of decreased activity of proline oxidase.
The analysis of the parameters regarding aerial parts highlights how Se-treated plants tend to recover their concentrations in Na, K, and Nprot (DS and WW plants) and in Fluo, Sulph, Phosph, and Chlor (only WW plants).
It is preferable not to hypothesize the causes of the increase of Na concentration in the analyzed plant material, because of its administration to the plant in the form of Na selenite. Interactions between Se and other elements, such as K, are also well-reported in literature. For example, Yao et al. (2013) documented that exogenous Se supply significantly enhanced the uptake of K in wheat, whereas, Pazurkiewicz-Kocot et al. (2003) noticed that Se supplementation increased K concentrations in maize grains. Indeed, Se is known to play important roles in inhibiting the production of ROS, which may be induced even by abiotic factors, such as DS. As the exposure to high levels of Se can possibly enhance membrane permeability, damage membrane integrity and produce high oxidative stress in treated plants, it was argued that the enhanced uptake of K might indicate that this element is involved in some mechanisms of Se tolerance within the plant (Feng et al., 2009).
Zahoor et al. (2017), reported that the increase of K in drought-stressed plants can sustain high nitrogen-metabolizing enzyme activities and contribute to osmotic adjustments in plants grown in soils under drought conditions.
The increase in Nprot concentrations, as a result of the Se-fortification, confirmed the results obtained by Ježek et al. (2011), when treating potato plants with foliar applications of sodium selenite. This increase is supposed to be another mechanism of resistance to an abiotic stress, induced by Se and implemented by the plant, which involves an increased intensity of amino acid metabolism.
As the increase in the concentration of Se in plants determines an increase in the concentration of K, which acts by limiting the damage due to DS inducing an increase in nitrogen metabolism, we can argue that Se itself induces tolerance toward DS.
The increase of the presence of anions, caused by Se-fortification of maize plants and which occurred only in good irrigation conditions. This may be related to the increased protein synthesis that may have induced an increase of the proteins that constitute the anion channel in the plasma membrane of cells, which are permeable to a range of physiological anions (Roberts, 2006), However, this hypothesis requires further confirmation.
In this paper, the MSAP technique was used in order to determine the level of DNA methylation in Z. mays under either water deficiency or Se treatment. The average of total relative cytosine methylation was 60.85% and was higher than that 26.15 and 32.15%, previously reported for maize leaves by Zhao et al. (2007) and Yang et al. (2011), respectively, but it was lower than 68.55% reported in the same species by Sun et al. (2015).
Positive effects of Se treatment were found to be associated with Se-mediated regulation of physiological and biochemical processes, such as increased chlorophyll and carotenoid concentrations and activation of antioxidant machinery in water stressed maize plants (Nawaz et al., 2016). Changes in DNA methylation could be considered a precise defensive mechanism to regulating the gene expression (Zhong et al., 2009).
In our study, the general methylation level of analyzed plants did not seem to be directly correlated with water stress and Se treatment, but it might be more influenced by genotype. In addition, Se supplementation seems to reduce the changes in DNA methylation caused by abiotic stress, probably due to its role in removing ROS produced by water stressed plant, as suggested by the low level of changes in methylation status in our samples. The protective role of Se against abiotic stress factors as high Cd concentration was also reported by Filek et al. (2008).
However, previous reports showed that environmental factors such as temperature, heavy metals and water stress as causing demethylation of genomic DNA (Chao et al., 2012). In fact, even if with small differences, methylation levels in water stressed plants without Se treatment were slightly higher than drought stressed plants with Se supplementation. These results seem to confirm that Se might reduce changes in methylation.
Among the few differentially methylated fragments, three were associated with known maize genes. In particular, ZM_1 displayed high similarity with a gene encoding for a chloroplast phytoene synthase (PSY1). Enzyme phytoene synthase catalyzes the conversion of two geranyl diphosphate in phytoene, which controls the flux of carotenoids. Carotenoids are necessary for photo protection and photosynthesis and they play an important role as a precursor to signaling molecules that influence plant development and biotic/abiotic stress responses. The gene family in maize and other grasses contains 3 paralogues. PSY1 is essential for maintaining leaf carotenoid content, particularly under heat stress growth conditions; the transcript level of PSY3 maize was regulated in response to abiotic stresses (Li et al., 2007), suggesting that PSY is involved in plant tolerance to abiotic stress (Han et al., 2008). In Pezzarossa et al. (2014), however, a reduction in β-carotene concentrations was also observed in tomato fortified with Se (1 mg Se L-1).
It had been reported that Se may down-regulate the expression of PSY, which was a key step of carotenoid biosynthesis in Arabidopsis (Sams et al., 2010). Moreover, Se was cited as down-regulating factor of some enzymes or genes of carotenoids synthesis in tomato (Pezzarossa et al., 2014).
ZM_2 displayed sequence homology with gene SDH. Plant SDH is the key enzyme in the sorbitol metabolism pathway (Nosarzewski and Archbold, 2007) and has been associated with resistance to abiotic stresses such as drought and salinity. SDH activity regulates the levels of polyols (Aguayo et al., 2013), which act as important osmolytes during DS and recovery processes.
ZM_3 displayed homology with gene encoding alcohol dehydrogenase 1 (ADH1). ADH activity may play a central role in biochemical adaptations to environmental stress. It is known to be induced during low oxygen stress, increasing in leaves and roots of plants exposed to flooding. In rice seeding, ADH1 and ADH2 are involved in flooding tolerance, but in maize and lettuce seedlings, the expression of genes is also responsive to wounding (Kato-Noguchi, 2001). The silencing of ADH in N. benthamiana and N. tabacum led to increased susceptibility of the plants to water deficit stress (Senthil-Kumar and Mysore, 2010).
As suggested by the methylation pattern of the fragments sequenced, Se did seem to bring back the methylation status. Indeed, in all the three bands the DS-Se caused changes in methylation status, while samples under DS treated by Se showed the same methylation pattern of controls.
We observed that maize plants responded to Se treatment by activating some physiological and biochemical changes, in order to cope with DS. The Se-biofortification treatment proved effective in increasing Se concentrations in maize roots and aerial parts. Regarding the drought stressed maize plants grown in Se-rich substrates, the increase of proline, K concentrations and nitrogen metabolism in aerial parts seems to prove that Se-biofortification increased the plant’s resistance to water shortage conditions. The increase of SeMeSeCys and SeCys2 forms in roots and aerial parts of Se-treated plants, suggests the induction of resistance strategies similar to those existing in Se-hyperaccumulator species.
Moreover, as SeMeSeCys is the form of Se which confers the best anticarcinogenic properties, this is advantageous from an animal and human nutrition perspective.
In addition, the MSAP technique was used to assess the level of DNA methylation/demethylation in maize plants under DS coupled with Se treatment. The methylation level in DS+Se plants was, even if with small differences, lower than that of (DS-Se) ones. In addition, the level of methylation of DS+Se plants was more similar to that of WW-Se plants, suggesting that Se could have a role in preventing and/or counteracting changes in methylation status.
RD, DB, and EA conceived the experiments and followed all the trials. MF, CP, GB, and RD performed the chemical analysis (selenium speciation, ionic concentrations, proline concentrations, and determination of total nitrogen). MB performed the MSAP experiments. SC and VN performed the statistical analysis for the molecular part. AO performed the statistical analysis for the chemical part. MB, RD, and SC wrote the manuscript. MB, RD, SC, VN, GM, DB, AO, and EA revised the manuscript.
The study was kindly supported by the University of Perugia (Italy) “Fondo di Ateneo per la Ricerca di Base 2015” (Italy), Project: Effect of selenium biofortification on resistance to water stress, vegetative growth and pollen performance in maize plants (Zea mays L.) (grant number: UNIPG_5_22_02_2017).
Conflict of Interest Statement
The authors declare that the research was conducted in the absence of any commercial or financial relationships that could be construed as a potential conflict of interest.
The Supplementary Material for this article can be found online at: https://www.frontiersin.org/articles/10.3389/fpls.2018.00389/full#supplementary-material
TABLE S1 | Instrumental settings of the ICP-MS and HPLC.
TABLE S2 | MSAP primer combination.
TABLE S3 | Moisture of aerial parts and roots. Length of aerial parts.
TABLE S4 | Principal component analysis, data.
TABLE S5 | DNA methylation level in maize plants subjected to drought stress or not, treated or not with selenium.
ADH, alcohol dehydrogenase; ANOVA, analysis of variance; CAT, catalase; DAS, days after sowing; DS, drought stress; GF-AAS, graphite furnace atomic adsorption spectroscopy; GPX, glutathione peroxidase; HPLC, high performance liquid chromatography; LSD, least significant difference; MSAP, methylation sensitive amplified polymorphism; NCBI, National Center for Biotechnology Information; PCA, principal component analysis; PCR, C-reactive protein; PSY, phytoene synthase; PVC, polyvinyl chloride; ROS, reactive oxygen species; SDH, sorbitol dehydrogenase; SOD, superoxide dismutase; TOPO, topoisomerase; WW, well-watered; ZM, Zea mays.
Abul-Soud, M. A., and Abd-Elrahman, S. H. (2016). Foliar selenium application to improve the tolerance of eggplant grown under salt stress conditions. Int. J. Plant Soil Sci. 9, 1–10. doi: 10.9734/IJPSS/2016/19992
Aguayo, M. F., Ampuero, D., Mandujano, P., Parada, R., Muñoz, R., Gallart, M., et al. (2013). Sorbitol dehydrogenase is a cytosolic protein required for sorbitol metabolism in Arabidopsis thaliana. Plant Sci. 20, 63–75. doi: 10.1016/j.plantsci.2013.01.012
Balal, R. M., Shahid, M. A., Javaid, M. M., Iqbal, Z., Anjum, M. A., Garcia-Sanchez, F., et al. (2016). The role of selenium in amelioration of heat-induced oxidative damage in cucumber under high temperature stress. Acta Physiol. Plant. 38, 1–14. doi: 10.1007/s11738-016-2174-y
Bocchini, M., Bartucca, M., Ciancaleoni, S., Mimmo, T., Cesco, S., Pii, Y., et al. (2015). Iron deficiency in barley plants: phytosiderophore release, iron translocation and DNA methylation. Front. Plant Sci. 6:514. doi: 10.3389/fpls.2015.00514
Broadley, M. R., Alcock, J., Alford, J., Cartwright, P., Foot, I., Fairweather-Tait, S. J., et al. (2010). Selenium biofortification of high-yielding winter wheat (Triticum aestivum L.) by liquid or granular Se fertilisation. Plant Soil 332, 5–18. doi: 10.1007/s11104-009-0234-4
Cartes, P., Jara, A. A., Pinilla, L., Rosas, A., and Mora, M. L. (2010). Selenium improves the antioxidant ability against aluminium-induced oxidative stress in ryegrass roots. Ann. Appl. Biol. 156, 297–307. doi: 10.1111/j.1744-7348.2010.00387.x
Cataldi, T. R. I., Margiotta, G., Del Fiore, A., and Bufo, S. A. (2003). Ionic content in plant extracts determined by ion chromatography with conductivity detection. Phytochem. Anal. 14, 176–183. doi: 10.1002/pca.700
Causevic, A., Delaunay, A., Ounnar, S., Righezza, M., Delmotte, F., Brignolas, F., et al. (2005). DNA methylating and demethylating treatments modify phenotype and cell wall differentiation state in sugarbeet cell lines. Plant Physiol. Biochem. 43, 681–691. doi: 10.1016/j.plaphy.2005.05.011
Chao, D. Y., Silva, A., Baxter, I., Huang, Y. S., Nordborg, M., Danku, J., et al. (2012). Genome-wide association studies identify heavy metal ATPase3 as the primary determinant of natural variation in leaf cadmium in Arabidopsis thaliana. PLoS Genet. 8:14. doi: 10.1371/journal.pgen.1002923
Chaoui, A., Mazhoudi, S., Ghorbal, M. H., and El Ferjani, E. (1997). Cadmium and zinc induction of lipid peroxidation and effects on antioxidant enzyme activities in bean (Phaseolus vulgaris L.). Plant Sci. 127, 139–147. doi: 10.1016/S0168-9452(97)00115-5
Chilimba, A. D., Young, S. D., Black, C. R., Meacham, M. C., Lammel, J., and Broadley, M. R. (2012). Agronomic biofortification of maize with selenium (Se) in Malawi. Field Crops Res. 125, 118–128. doi: 10.1016/j.fcr.2011.08.014
Cubadda, F., Aureli, F., Ciardullo, S., D’Amato, M., Raggi, A., Acharya, R., et al. (2010). Changes in selenium speciation associated with increasing tissue concentration of selenium in wheat grain. J. Agric. Food Chem. 58, 2295–2301. doi: 10.1021/jf903004a
De Souza, M. P., Pilon-Smits, E. A. H., Lytle, C. M., Hwang, S., Tai, J., Honma, T. S., et al. (1998). Rate-limiting steps in selenium assimilation and volatilization by Indian Mustard. Plant Physiol. 117, 1487–1494. doi: 10.1104/pp.117.4.1487
Dong, J. Z., Wang, Y., Wang, S. H., Yin, L. P., Xu, G. J., Zheng, C., et al. (2013). Selenium increases chlorogenic acid, chlorophyll and carotenoids of Lycium chinense leaves. J. Sci. Food Agric. 93, 310–315. doi: 10.1002/jsfa.5758
Elkahoui, S., Smaoui, A., Zarrouk, M., Ghrir, R., and Limam, F. (2004). Salt-induced lipid changes in Catharanthus roseus cultured cell suspensions. Phytochemistry 65, 1911–1917. doi: 10.1016/j.phytochem.2004.06.021
Filek, M., Keskinen, R., Hartikainen, H., Szarejko, I., Janiak, A., Miszalski, Z., et al. (2008). The protective role of selenium in rape seedlings subjected to cadmium stress. J. Plant Physiol. 165, 833–844. doi: 10.1016/j.jplph.2007.06.006
Han, H., Li, Y., and Zhou, S. (2008). Overexpression of phytoene synthase gene from Salicornia europaea alters response to reactive oxygen species under salt stress in transgenic Arabidopsis. Biotechnol. Lett. 30, 1501–1507. doi: 10.1007/s10529-008-9705-6
Hanson, B., Lindblom, S. D., Loeffler, M. L., and Pilon-Smits, E. A. (2004). Selenium protects plants from phloem-feeding aphids due to both deterrence and toxicity. New Phytol. 162, 655–662. doi: 10.1111/j.1469-8137.2004.01067.x
Hasanuzzaman, M., and Fujita, M. (2011). Selenium pretreatment upregulates the antioxidant defense and methylglyoxal detoxification system and confers enhanced tolerance to drought stress in rapeseed seedlings. Biol. Trace Elem. Res. 143, 1758–1776. doi: 10.1007/s12011-011-8998-9
Hawrylak-Nowak, B., Matraszek, R., and Pogorzelek, M. (2015). The dual effects of two inorganic selenium forms on the growth, selected physiological parameters and macronutrients accumulation in cucumber plants. Acta Physiol. Plant 37, 1–13. doi: 10.1007/s11738-015-1788-9
Ježek, P., Hlušek, J., Lošák, T., Jůzl, M., Elzner, P., Kráčmar, S., et al. (2011). Effect of foliar application of selenium on the content of selected amino acids in potato tubers (Solanum tuberosum L.). Plant Soil Environ. 57, 315–320. doi: 10.17221/57/2011-PSE
Khan, M. I. R., Nazir, F., Asgher, M., Per, T. S., and Khan, N. A. (2015). Selenium and sulfur influence ethylene formation and alleviate cadmium-induced oxidative stress by improving proline and glutathione production in wheat. J. Plant Physiol. 173, 9–18. doi: 10.1016/j.jplph.2014.09.011
Li, H.-F., McGrath, S. P., and Zhao, F.-J. (2008). Selenium uptake, translocation and speciation in wheat supplied with selenate or selenite. New Phytol. 178, 92–102. doi: 10.1111/j.1469-8137.2007.02343.x
Li, M. Q., Hasan, M., Li, C. X., Ahammed, G. J., Xia, X. J., Shi, K., et al. (2016). Melatonin mediates selenium-induced tolerance to cadmium stress in tomato plants. J. Pineal Res. 61, 291–302. doi: 10.1111/jpi.12346
Lichtenthaler, H. K., and Wellburn, A. R. (1983). Determinations of total carotenoids and chlorophylls a and b of leaf extracts in different solvents. Biochem. Soc. Trans. 11, 591–592. doi: 10.1042/bst0110591
Lukens, L. N., and Zhan, S. (2007). The plant genome’s methylation status and response to stress: implications for plant improvement. Curr. Opin. Plant Biol. 10, 317–322. doi: 10.1016/j.pbi.2007.04.012
Marconi, G., Pace, R., Traini, A., Raggi, L., Lutts, S., Chiusano, M., et al. (2013). Use of MSAP markers to analyse the effects of salt stress in DNA methylation in rapessed (Brassica napus var. oleifera). PloS One 8:e75597. doi: 10.1371/journal.pone.0075597
Nawaz, F., Ahmad, R., Ashraf, M. Y., Waraich, E. A., and Khan, S. Z. (2015). Effect of selenium foliar spray on physiological and biochemical processes and chemical constituents of wheat under drought stress. Ecotoxicol. Environ. Saf. 113, 191–200. doi: 10.1016/j.ecoenv.2014.12.003
Nawaz, F., Naeem, M., Ashraf, M. Y., Tahir, M. N., Zulfiqar, B., Salahuddin, M., et al. (2016). Selenium supplementation affects physiological and biochemical processes to improve fodder yield and quality of maize (Zea mays L.) under water deficit conditions. Front. Plant Sci. 7:1438. doi: 10.3389/fpls.2016.01438
Palmerini, C. A., Vedovelli, A., Morelli, A., Fini, C., and Floridi, A. (2006). Analysis of acid-soluble hydroxy-proline, free proline and collagen-bound hydroxyproline in rat liver by high performance liquid chromatography with pre-column derivatization. J. Liq. Chromatogr. 8, 1853–1868. doi: 10.1080/01483918508074100
Pandey, R. K., Maranville, J. W., and Admou, A. (2000). Deficit irrigation and nitrogen effects on maize in a Sahelian environment: I. Grain yield and yield components. Agric. Water Manae. 46, 1–13. doi: 10.1016/S0378-3774(00)00073-1
Pazurkiewicz-Kocot, K., Galas, W., and Kita, A. (2003). The effect of selenium on the accumulation of some metals in Zea mays L. plants treated with indole-3-acetic acid. Cell. Mol. Biol. Lett. 8, 97–103.
Peng, H., and Zhang, J. (2009). Plant genomic DNA methylation in response to stresses: potential applications and challenges in plant breeding. Prog. Nat. Sci. 19, 1037–1045. doi: 10.1016/jpnsc.2008.10.014
Pezzarossa, B., Rosellini, I., Borghesi, E., Tonutti, P., and Malorgio, F. (2014). Effects of Se-enrichment on yield, fruit composition and ripening of tomato (Solanum lycopersicum) plants grown in hydroponics. Sci. Hortic. 165, 106–110. doi: 10.1016/j.scienta.2013.10.029
Pilon-Smits, E. A. H., and Quinn, C. F. (2010). “Selenium metabolism in plants,” in Cell Biology of Metals and Nutrients, Plant Cell Monographs, Vol. 17, eds R. Hell and R.-R. Mendel (Berlin: Springer-Verlag), 225–241. doi: 10.1007/978-3-642-10613-2_10
Proietti, P., Nasini, L., Del Buono, D., D’Amato, R., Tedeschini, E., Businelli, D., et al. (2013). Selenium protects olive (Olea europaea L.) from drought stress. Sci. Hortic. 164, 165–171. doi: 10.1016/j.scienta.2013.09.034
Rotruck, J. T., Pope, A. L., Ganther, H. E., Swanson, A. B., Hafeman, D. G., and Hoekstra, W. (1973). Selenium: biochemical role as a component of glutathione peroxidase. Science 179, 588–590. doi: 10.1126/science.179.4073.588
Sams, C. E., Panthee, D. R., Charron, C. S., Kopsell, D. A., and Yuan, J. S. (2010). Selenium regulates gene expression for glucosinolate and carotenoid biosynthesis in Arabidopsis. J. Am. Soc. Hortic. Sci. 136, 23–34.
Senthil-Kumar, M., and Mysore, K. S. (2010). Assessing functional role of three water deficit stress-induced genes in nonhost disease resistance using virus-induced gene silencing in Nicotiana benthamiana. Plant Signal. Behav. 5, 586–590. doi: 10.4161/psb.11497
Sun, L. F., Liu, T. J., Shan, X. H., Su, S. Z., Li, S. P., Yuan, Y. P., et al. (2015). Analysis of DNA cytosine methylation patterns in maize hybrids and their parents. Biol. Plant. 59, 266–272. doi: 10.1007/s10535-015-0490-5
Teyssier, E., Bernacchia, G., Maury, S., Kit, A. H., Stammitti-Bert, L., Rolin, D., et al. (2008). Tissue dependent variations of DNA methylation and endoreduplication levels during tomato fruit development and ripening. Planta 228, 391–399. doi: 10.1007/s00425-008-0743-z
Valkama, E., Kivimäenpää, M., Hartikainen, H., and Wulff, A. (2003). The combined effects of enhanced UV-B radiation and selenium on growth, chlorophyll fluorescence and ultrastructure in strawberry (Fragaria X ananassa) and barley (Hordeum vulgare) treated in the field. Agric. Forest Meteorol. 120, 267–278. doi: 10.1016/j.agrformet.2003.08.021
Wang, Y. D., Wang, X., and Wong, Y. S. (2013). Generation of selenium-enriched rice with enhanced grain yield, selenium content and bioavailability through fertilisation with selenite. Food Chem. 141, 2385–2393. doi: 10.1016/j.foodchem.2013.05.095
Ximénez-Embún, P., Alonso, I., Madrid-Albarrán, Y., and Cámara, C. (2004). Establishment of selenium uptake and species distribution in lupine, Indian mustard, and sunflower plants. J. Agric. Food Chem. 52, 832–838. doi: 10.1021/jf034835f
Yang, W., Yu, X., and Liu, B. (2011). Parental epigenetic difference in DNA methylation-level may play contrasting roles for different agronomic traits related to yield heterosis in maize. Afr. J. Biotechnol. 10, 9253–9263. doi: 10.5897/AJB11.298
Yao, X., Jianzhou, C., Xueli, H., Binbin, L., Jingmin, L., and Zhaowei, Y. (2013). Effects of selenium on agronomical characters of winter wheat exposed to enhanced Ultra-Violet-B. Ecotoxicol. Environ. Saf. 92, 320–326. doi: 10.1016/j.ecoenv.2013.03.024
Zahoor, R., Zhao, W., Abid, M., Dong, H., and Zhou, Z. (2017). Potassium application regulates nitrogen metabolism and osmotic adjustment in cotton (Gossypium hirsutum L.) functional leaf under drought stress. J. Plant Physiol 215, 30–38. doi: 10.1016/j.jplph.2017.05.001
Zhang, L.-H., Abdel-Ghany, S. E., Freeman, J. L., Ackley, A. R., Schiavon, M., and Pilon-Smits, E. A. H. (2006). Investigation of selenium tolerance mechanisms in Arabidopsis thaliana. Physiol. Plant 128, 212–223. doi: 10.1111/j.1399-3054.2006.00739.x
Zhao, X., Chai, Y., and Liu, B. (2007). Epigenetic inheritance and variation of DNA methylation level and pattern in maize intra-specific hybrids. Plant Sci. 172, 930–938. doi: 10.1016/j.plantsci.2007.01.002
Keywords: selenium, maize, selenium speciation, water stress, DNA methylation, epigenetic
Citation: Bocchini M, D’Amato R, Ciancaleoni S, Fontanella MC, Palmerini CA, Beone GM, Onofri A, Negri V, Marconi G, Albertini E and Businelli D (2018) Soil Selenium (Se) Biofortification Changes the Physiological, Biochemical and Epigenetic Responses to Water Stress in Zea mays L. by Inducing a Higher Drought Tolerance. Front. Plant Sci. 9:389. doi: 10.3389/fpls.2018.00389
Received: 17 November 2017; Accepted: 09 March 2018;
Published: 27 March 2018.
Edited by:Victoria Fernandez, Universidad Politécnica de Madrid (UPM), Spain
Reviewed by:Garcia-Sanchez Francisco, Centro de Edafología y Biología Aplicada del Segura (CSIC), Spain
Ferenc Fodor, Eötvös Loránd University, Hungary
Copyright © 2018 Bocchini, D’Amato, Ciancaleoni, Fontanella, Palmerini, Beone, Onofri, Negri, Marconi, Albertini and Businelli. This is an open-access article distributed under the terms of the Creative Commons Attribution License (CC BY). The use, distribution or reproduction in other forums is permitted, provided the original author(s) and the copyright owner are credited and that the original publication in this journal is cited, in accordance with accepted academic practice. No use, distribution or reproduction is permitted which does not comply with these terms.
*Correspondence: Emidio Albertini, email@example.com