Xiaoyan He†
Yaru He†Yihuan Dong†Yu GaoXingcai SunWeiyue ChenXintong XuCongjun SuYifan LvBoyu RenHuayan YinJianbin ZengWujun Ma
Ping Mu*- College of Agronomy, Qingdao Agricultural University, Qingdao, China
FHY3 and its homologous protein FAR1 are the founding members of FRS family. They exhibited diverse and powerful physiological functions during evolution, and participated in the response to multiple abiotic stresses. FRF genes are considered to be truncated FRS family proteins. They competed with FRS for DNA binding sites to regulate gene expression. However, only few studies are available on FRF genes in plants participating in the regulation of abiotic stress. With wide adaptability and high stress-resistance, barley is an excellent candidate for the identification of stress-resistance-related genes. In this study, 22 HvFRFs were detected in barley using bioinformatic analysis from whole genome. According to evolution and conserved motif analysis, the 22 HvFRFs could be divided into subfamilies I and II. Most promoters of subfamily I members contained abscisic acid and methyl jasmonate response elements; however, a large number promoters of subfamily II contained gibberellin and salicylic acid response elements. HvFRF9, one of the members of subfamily II, exhibited a expression advantage in different tissues, and it was most significantly upregulated under drought stress. In-situ PCR revealed that HvFRF9 is mainly expressed in the root epidermal cells, as well as xylem and phloem of roots and leaves, indicating that HvFRF9 may be related to absorption and transportation of water and nutrients. The results of subcellular localization indicated that HvFRF9 was mainly expressed in the nuclei of tobacco epidermal cells and protoplast of arabidopsis. Further, transgenic arabidopsis plants with HvFRF9 overexpression were generated to verify the role of HvFRF9 in drought resistance. Under drought stress, leaf chlorosis and wilting, MDA and O2− contents were significantly lower, meanwhile, fresh weight, root length, PRO content, and SOD, CAT and POD activities were significantly higher in HvFRF9-overexpressing arabidopsis plants than in wild-type plants. Therefore, overexpression of HvFRF9 could significantly enhance the drought resistance in arabidopsis. These results suggested that HvFRF9 may play a key role in drought resistance in barley by increasing the absorption and transportation of water and the activity of antioxidant enzymes. This study provided a theoretical basis for drought resistance in barley and provided new genes for drought resistance breeding.
1 Introduction
FAR-RED ELONGATED HYPOCOTYL 3 (FHY3) and its homologous protein FAR-RED IMPAIRED RESPONSE 1 (FAR1) are important optical signaling proteins involved in the transduction of far-red light signals and are a new class of transcription factors evolved from the ancient Mutator transposases (Hudson et al., 1999; Wang and Deng, 2002). They can specifically recognize the cis-regulatory element FBS and further regulate the transcription level of multiple downstream target genes (Liu et al., 2017). FHY3/FAR1 are essentially the founding members of FAR1-RELATED SEQUENCE (FRS) family, which are conserved in terrestrial plants. Most members of the FRS family have an N-terminal C2H2 zinc finger domain (FAR1 DNA-binding domain), a central transposase domain similar to MULE transposases, and a C-end SWIM zinc finger structural domain (Lin et al., 2007). FRS-RELATED FACTOR (FRF) genes are considered to be truncated FRS family proteins because they only contain the FAR1 DNA-binding domain but not the presumed core transposase and C-end SWIM domain (Aguilar-Martínez et al., 2015). It is proposed that FRF can compete with FRS for the DNA binding sites of its targets or regulate the transcription factors of target genes by interacting with other transcription factors (Aguilar-Martínez et al., 2015). However, the underlying molecular mechanisms of this gene family need to be further studied.
The FRS and FRF families of arabidopsis (Arabidopsis thaliana) have 18 members, including FHY3 and FAR1, as well as 12 FRS and 4 FRF proteins (Lin and Wang, 2004; Ma and Li, 2018). Multiple sequence alignment (MSA) and conserved protein motif analysis revealed that FRS and FRF family proteins in arabidopsis can be divided into six subfamilies. Generally, most FRS and FRF family proteins have a DNA-binding domain at their N-end region. However, as an exception, AtFRS7 and AtFRS12 have two DNA-binding domains; AtFRS9 has no DNA-binding domain at the N-end but only the MULE core transposase domain, and AtFRF1–AtFRF4 contain only the N-end FAR1 DNA-binding domain (Ma and Li, 2018).
For the function of FRS and FRF gene families, research mainly focuses on FHY3/FAR1. Although FHY3/FAR1 are derived from transposase, they have evolved diverse and powerful physiological functions during adaptation and domestication including light signal transduction and light morphogenesis (Lin et al., 2007), chloroplast division and chlorophyll biosynthesis (Ouyang et al., 2011), circadian clock and flowering time regulation (Li et al., 2011), shoot apex meristem and flower development (Joly-Lopez et al., 2016; Li et al., 2016), starch synthesis and starch granule formation (Ma et al., 2017), abscisic acid (ABA) signaling and stress response (Tang et al., 2013), oxidative stress and plant immune response (Ma et al., 2016; Wang et al., 2016), and nutrient uptake (Ma and Li, 2021). This indicates that this class of genes is essential for plant growth, development, and stress resistance. For example, FHY3/FAR1 negatively regulated accumulation of reactive oxygen species (ROS) and oxidative-stress-induced cell death, and fhy3 and far1 mutant plants grew slowly and displayed severe cell death under the conditions of short days or long periods of darkness (Stirnberg et al., 2012; Ma et al., 2016; Wang et al., 2016). Loss of FHY3/FAR1 function enhanced expression of defense-response genes and thus increased the tolerance to Pseudomonas syringae, indicating that FHY3 and FAR1 are also involved in plant immune regulation (Wang et al., 2016). ABA plays various important roles in plant growth and development, including grain maturation, germination, and stress response (Chen K. et al., 2020). fhy3 mutant plants were less sensitive to salt and osmotic stresses than the wild-type plants. In addition, mutant plants with disrupted FHY3/FAR1 function were less sensitive to ABA-induced stomatal motility, suggesting that FHY3/FAR1 are required for stomatal motility and drought response in plants (Tang et al., 2013). Additionally, the transcript level of ABA INSENSITIVE5 (ABI5) was decreased in fhy3, far1, and fhy3/far1 mutant plants, and after ABI5 overexpression, the phenotype of fhy3 mutant plants was similar to that of the wild-type plants. These results indicated that ABI5 is regulated by FHY3 and FAR1 (Tang et al., 2013; Xu et al., 2020). Therefore, FHY3 and FAR1 bind to the ABI5 promoter and activate its transcription, thereby mediating ABA signaling and abiotic stress responses.
Currently, there are also some research reports on FRS. Over 1000 FRS homologs have been successively predicted in various higher plant species (Lin et al., 2007; Joly-Lopez et al., 2016). FRS10, which was screened based on Silver birch genome sequencing and population genome, may play a regulatory role in the adaptability of plants to the environment (Salojärvi et al., 2017). Some predicted FRS family members may be the candidates for the regulation of panniculus and spiky degeneration in rice (Zhang et al., 2015), as well as photoperiod-dependent flowering time regulators in wheat (Kiseleva et al., 2017). However, the physiological functions and molecular mechanisms of FRF family proteins in higher plants remain largely unknown.
Drought is one of the most serious abiotic stresses affecting normal plant growth and limiting crop yield worldwide. Barley (Hordeum vulgare L.) is one of the oldest diploid crops in the world. It is suitable for cultivation at high altitude and cold temperature and in arid, saline–alkali, and barren land (Carter et al., 2019; Kebede et al., 2019). Therefore, it is an important plant material for exploring excellent stress-resistance genes, including drought-resistant genes. It is of great significance to clarify the drought-resistant mechanisms in barley for developing new methods to resist drought stress and improving the yield of barley and other plants. In this study, we aimed to identify drought-resistance-related FRF genes from barley. The FRF gene family was identified in barley from whole genome, and the drought response gene HvFRF9 was screened and its function in drought resistance was verified. This study provided a theoretical basis for drought resistance in barley and provided new genes for drought resistance breeding.
2 Materials and methods
2.1 Identification of FRF genes in barley
Genomic data, CDS, protein files, and gff3 annotation files of barley Morex were downloaded from the Barley IPK database (https://galaxy-web.ipk-gatersleben.de/). The FRF sequences containing only FAR1 domain (PF03101) were searched in the Barley Protein database with a search threshold of E value < 1e−10 using Hmmer-search 3.0 program. The preliminary barley FRF protein sequence was submitted to SMART (http://smart.embl-heidelberg.de/), NCBI-CDD (https://www.ncbi.nlm.nih.gov/cdd/), and PFAM website (http://pfam.xfam.org/) to ensure the complete FAR1 domain structure. After removing suspicious sequences, the HvFRF gene family members were obtained. The protein sequences of HvFRF family members were uploaded to the Expasy (https://web.expasy.org) website, and their molecular weight (MW) and isoelectric point (pI) were predicted.
2.2 Construction of phylogenetic tree for HvFRFs
The FRF sequence of A. thaliana was downloaded from TAIR, the arabidopsis genome website (https://www.arabidopsis.org/index.jsp). The Triticum aestivum L. (wheat), Brachypodium distachyon L. (brachypodium), Zea mays L. (corn), Oryza sativa L. (rice), Sorghum bicolor L. (sorghum), Glycine max L. (soybean), and Vitis vinifera L. (grape) protein databases were downloaded from the Ensemble Plants website (http://plants.ensembl.org/index.html). The FRF genes containing FAR1 domain but not MULE and SWIM zinc finger structural domain were searched from wheat, brachypodium, maize, rice, sorghum, soybean, and grape protein databases using Hmmer-search 3.0 program with E value < 1e−10 and Blastp program based on four FRF member sequences in arabidopsis. The FRF protein sequences obtained from the preliminary screening were submitted to SMART, NCBI-CDD, and PFAM websites to further confirm the integrity of FAR1 domain and obtain FRF gene family information in the above species. MSAs were performed using Clustal W to analyze the evolutionary relationships between HvFRF gene family members and FRF proteins in brachypodium, soybean, grape and arabidopsis. Phylogenetic tree was constructed using Neighbor-joining method, and the bootstrap value was set to 1000 replicates. The evolutionary tree was edited using the iTOL 2.0 website (https://itol.embl.de/).
2.3 Chromosomal localization and gene duplication event analysis of HvFRFs
Tbtools software (Chen C. et al., 2020) was used to obtain the chromosome length, gene density, and chromosome location information of HvFRF genes from the barley genome database, and the chromosome location map of HvFRFs was drawn. Members of the HvFRF family were named according to the order of their physical positions on seven chromosomes. MCScanX software was used to analyze the gene duplication events in the barley genome and HvFRF family. The extracted gene collinearity results were combined with barley chromosome gene density and visualized using Tbtools to generate a collinearity map of FRF gene families within barley species.
2.4 Conserved motifs, gene structure, cis-elements and upstream IF and miRNA analysis of HvFRFs
MEME online tool (http://meme-suite.org/) was used to analyze the conserved motifs of HvFRF proteins, with the number of conserved motifs set as 5 and the width of motifs set as 6–150. The genetic structure of HvFRFs was analyzed using GSDS (http://gsds.cbi.pku.edu.cn/). The obtained files were imported into TBtools software for visualization. TBtools software was used to extract the sequence 2000-bp upstream of ATG of HvFRF gene family. It was submitted to PlantCARE website (http://bioinformatics.psb.ugent.be/webtools/plantcare/html/) for promoter cis-element analysis. The analysis results were collated and imported into TBtools for visualization. The transcription factor (IF) binding site within the promoter regions of HvFRF genes were predicted through the online PlantRegMap tool (http://plantregmap.gao-lab.org/binding_site_prediction.php), where the species was set to Hordeum vulgare L. The upstream miRNAs of HvFRFs were predicted using psRNATarget (https://www.zhaolab.org/psRNATarget/analysis?function=2). The main parameters were set as follows: the penalty for G:U pair was 0.5, the number of mismatches allowed in the seed region was 2, the penalty for opening gap was 2, and the penalty for extending gap was 0.5.
2.5 Tissue expression profile and expression characteristics of HvFRFs in response to drought
The expression levels of 22 HvFRF genes in various barley tissues such as root, epidermal cells, inflorescence, and grain at various growth stages were downloaded from WheatOmics 1.0 (http://202.194.139.32/) database. TBtools software was used to plot the heat map.
The grains of Golden Promise variety of barley with consistent grain size were selected and sterilized with 75% alcohol before germination on a filter paper. Seven days after germination, seedlings with consistent growth were selected and transferred to 5-L black plastic drums containing 1/5 Hoagland nutrient solution for further cultivation (16 h/8 h, 23°C/18°C, day/night). The nutrient solution was changed every 2–3 days during seedling growth stage, and the pH of the nutrient solution was maintained at 5.8–6.0 with continuous ventilation. When the seedlings grew to two-leaves and one-heart stage, drought stress was simulated with 15% (15 g/100 ml) PEG6000 on three biological replicates. After 1, 3, 6, 12, 24, and 48 h of drought stress treatment, the roots were cooled in liquid nitrogen and used for RNA extraction. Total RNA was extracted from the roots using SteadyPure Plant RNA Extraction Kit (Accurate Biology Co., Qingdao, China). cDNA was obtained using Evo M-MLV Reverse Transcription Kit for qPCR (Accurate Biology Co., Qingdao, China). Fluorescence quantification experiments were performed using SYBR Green Pro Taq HS Premixed type Kit (Accurate Biology Co., Qingdao, China). The PCR program used a two-step method: 95°C for 30 s, followed by 40 cycles of 95°C for 5 s and 60°C for 30 s. Relative HvFRFs expression values were calculated using the 2−ΔΔCt relative quantification method. The primers used for qRT-PCR are given in Supplementary Table S1.
2.6 Cloning and sequence analysis of HvFRF9
RNA and DNA were extracted from the roots of hydroponically grown Golden Promise barley at two-leaves and one-heart stage without any treatment, and full length cDNA was generated by reverse transcription using Evo M-MLV Plus cDNA synthesis kit (Accurate Biology Co., Qingdao, China). Gene cloning primers HVFRF9-F and HVFRF9-R (Supplementary Table S1) were designed using Primer 5.0 to amplify the full-length open reading frame (ORF) of the HvFRF9 gene using cDNA and DNA as templates, respectively. The amplified and purified fragments were ligated into pEASY-Blunt vector. The ligation products were used to transform competent Escherichia coli Trans1-T1 cells, which were cultured overnight at 37°C on LB solid medium containing 100 mg/L ampicillin (Amp). The positive clones detected using PCR were sent to Tsingke Biotech Co., Ltd. (Beijing, China) for sequencing, and the plasmids of the correctly sequenced clones were used to obtain intermediate vector pEASY-Blunt-HVFRF9.
The nucleotide sequence of HvFRF9 gene was translated into amino acid sequences using BioXM 2.7, and the amino acid sequences were analyzed using SMART to confirm the functional domain. The HvFRF9 protein sequence was compared with that of four arabidopsis FRF members (AtFRF1, AtFRF2, AtFRF3, and AtFRF4) using DNAMAN software. The secondary structure of HvFRF9 was predicted using PSIPRED (http://bioinf.cs.ucl.ac.uk/psipred), and its three dimensional (3D) structure was builded using SWISS-MODEL (https://swissmodel.expasy.org/interactive).
2.7 Analysis of the expression site of HvFRF9 using in-situ PCR
In-situ PCR of HvFRF9 was performed according to the method described by Athman (Athman et al., 2014). From the hydroponically cultured Golden Promise, the roots and leaves at the two-leaves and one-heart stage were collected, immediately placed in fresh formaldehyde fixative (63 ml/100 ml Ethanol, 5 ml/100 ml acetic acid, 2 ml/100 ml formaldehyde). Each tissue was embedded in 5% agarose. The embedded tissue sections (60–70 μm for leaves and 50 μm for roots) were subjected to a vibrating microtome (ZQP-86, Zhixin, Shanghai, China). Each cut tissue sample was placed into a PCR tube, treated with DnaseI, and reverse transcribed for in-situ PCR studies. The transintron-specific primers were designed for HvFRF9 (in-situ-HvFRF9-F and in-situ-HvFRF9-R; Table S1), and the gene was amplified with digoxigenin-labeled dUTP using each tissue section as a template. Anti-DIG AP antibody was added to the PCR products, incubated at 37°C for 1 h, and washed twice with the wash buffer (0.1 M Tris-HCl, 0.15 M NaCl, pH = 9.5). BM-Purple was added for staining. Further, the samples were thoroughly washed with the wash buffer and placed on slides to observe the expression site of HvFRF9 in the roots and leaves under a positive fluorescence microscope (DM6B, Leica, Wetzlar, Germany). 18S rRNA gene was used as a positive control, and the sample without primers served as a negative control.
2.8 Subcellular localization of HvFRF9
The coding sequence of HvFRF9 gene (stop codon removed) was amplified using the intermediate vector, pEASY-Blunt-HvFRF9, and ligated into SUPER1300-35S-GFP and P131-35S-YFP vectors, respectively. The ligation products were used to transform competent E. coli Trans1-T1 cells, and positive clones were obtained and sequenced. SUPER1300-35S-HvFRF9-GFP and P131-35S-HvFRF9-YFP of subcellular localization vector were obtained from the plasmids of the correctly sequenced clones (to ensure that there was no frame shift and the complete fusion protein could be translated). SUPER1300-35S-HvFRF9-GFP, nuclear localization marker, arabidopsis protoplasts, and PEG4000 solution were mixed and placed in water bath for 15 min. Protoplasts were collected after washing with W5 solution (154 mM NaCl, 125 mM CaCl2, 5 mM KCl, 5 mM glucose, and 2 mM MES). The fluorescence distribution was observed under a laser confocal microscope (A1 HD25, Nikon, Tokyo, Japan). P131-35S-HvFRF9-YFP plasmid was transferred into Agrobacterium tumefaciens EHA105, which was used to infect tobacco (Nicotiana benthamiana) at the 4–5 leaf stage. Between 36 and 72 h after infection, undamaged tobacco leaves were selected to make sample slides. The fluorescence distribution was observed under a laser confocal microscope (A1 HD25, Nikon, Tokyo, Japan). The culture conditions for tobacco were 24°C/26°C, 16 h/8 h, day/night.
2.9 Establishment of overexpression carrier of HvFRF9 and genetic transformation of arabidopsis
The overexpression primers HvFRF9-OE-F and HvFRF9-OE-R (Supplementary Table S1) were designed using Primer 5.0, and the coding sequence (with stop codon) of HvFRF9 gene was amplified from the intermediate vector pEASY-Blunt-HvFRF9 and connected to the SUPER1300 vector. The ligation product was used to transform competent E. coli Trans1-T1 cells. Positive clones were obtained and sequenced. The cloned plasmids with correct sequencing were used to obtain the overexpression carrier SUPER1300-35S-HvFRF9. This recombinant plasmid was used to transform A. tumefaciens GV3101. The transformed bacterial cells were grown in liquid YEB medium containing rifampicin (20 mg/L) and kanamycin (50 mg/L) on a shaker till OD600 of 1.2 was obtained. The cells were collected by centrifugation at 5000 g and resuspended in osmotic buffer (5 g/100 mL sucrose, 20 μL/100 mL Silwet L-77, 0.05 g/100 mL 1/2 MS) to obtain the inoculum for infection with the OD600 of 0.8–1.0. The flower bud parts of wild-type arabidopsis (Col-0) were inoculated with the inoculum for infection, and the seeds of the T1 generation were harvested when arabidopsis plants were mature. The seeds of T1 generation were disinfected and seeded in solid medium containing 25 mg/L hygromycin, from which the seedlings with developed roots and strong growth were selected for further cultivation. The seeds of T2 generation were harvested from each plant, and These seeds were further grown on culture medium with 25 mg/L hygromycin, and strains with a 3:1 separation ratio between positive and negative seedlings were selected to verify the expression level of HvFRF9 gene. The primer information is given in Supplementary Table S1. Three lines with high expression levels were selected, and T3 grains were harvested from each plant to obtain the HvFRF9 overexpression lines. Arabidopsis culture conditions were as follows: 23°C, 16 h/8 h, day/night.
2.10 Identification of drought-resistant phenotypes of arabidopsis with HvFRF9 overexpression
Wild-type and HvFRF9-overexpressing arabidopsis grains were sterilized and planted on 1/2 MS solid medium without antibiotics. After 3 days of vernalization, the medium was placed in a light incubator (23°C, 16 h/8 h, day/night). After 1 week, the seedlings with consistent growth were selected and transferred to MS solid medium containing various concentrations of mannitol (0, 50, 100, and 200 mM). Three biological replicates were used for each treatment. After 1 week, the main root length of arabidopsis was observed and measured, and the fresh weight of each line was determined.
Wild-type and HvFRF9-overexpressing arabidopsis seedlings grown normally for 1 week on 1/2 MS solid medium were transferred to 0.2-L seedling pots for continued cultivation (23°C, 16 h/8 h, day/night), each containing nutrient soil of equal weight and humidity. Drought treatment was performed as follows after 3 days of culture. The control group was watered normally (keeping the soil water content at 80% ± 5%), and the drought group did not receive water. Three biological replicates with six plants per replicate were used in the control and drought groups. After 14 days of drought treatment, the phenotypes of arabidopsis were observed, and the physiological parameters were measured. The superoxide anion (O2−) activity in the leaves of arabidopsis was measured using NBT method (Bournonville and Diaz-Ricci, 2011). Malondialdehyde (MDA) and proline (PRO) contents in the leaves were determined using MDA and PRO Content Assay Kits (Solarbio Science & Technology Co., Ltd., Beijing, China), respectively. Catalase (CAT), superoxide dismutase (SOD), and peroxidase (POD) activities in the leaves were determined using CAT assay kit (Visible light), SOD assay kit (WST-1 method), and POD assay kit (Nanjing Jiancheng Bioengineerring Institute, Nanjing, China), respectively.
2.11 Data analysis
IBM SSPS Statistics 22 software was used for the statistical analysis of data. The significance of difference (p < 0.05) was tested by least-significant difference using one-way ANOVA, and the significance of data was marked by Waller–Duncan letter labeling method (p < 0.05).
3 Results
3.1 Identification of FRF genes in barley and analysis of their physicochemical properties
A total of 52 candidate FAR1-domain-containing genes were identified in the genome-wide data of barley. In total, 22 FRF family proteins were identified using SMART, NCBI-CDD, and PFAM. The 22 HvFRFs were named HvFRF1–HvFRF22 (Table 1) based on their positional order on barley chromosomes. The physicochemical properties of HvFRF proteins were analyzed. The number of amino acids ranged from 189–399 aa, with an average of 240.9 aa. The MW ranged from 21.6–45.7 kDa, with an average of 27.9 kDa. The pI ranged from 5.09–10.67, with an average of 8.83. Moreover, 86% of the proteins had pI > 7, indicating that the proteins in this family were slightly alkaline (Table 1).
Table 1 Basic information of HvFRF gene family in barley.
3.2 Phylogenetic tree of HvFRF gene family
To screen and identify FRF genes in the genomes of monocotyledonous grasses such as wheat, brachypodium, corn, rice, and sorghum and dicotyledonous plants such as soybean and grape, four FRF (FRF1–FRF4) protein sequences in Arabidopsis were used. The FRF genes containing only the FAR1 domain but not the MULE domain and SWIM zinc finger structural domain were searched from the protein databases of the seven species mentioned above using the Hmmer-search 3.0 and the Blastp programs. In total, 17 BdFRF, 21 GmFRF and 11 VvFRF genes were identified from brachypodium, soybean and grape genomes, respectively. It can be seen that the number of FRF genes in barley was almost the same, twice, and 5 times that of FRF genes in soybean, brachypodium, grape, and arabidopsis, respectively. Nevertheless, FRF members were not found in the genomes of wheat, corn, rice, and sorghum, which are the grasses similar to barley.
The protein sequences of 22 barley HvFRF genes, 17 brachypodium BdFRF genes, 21 soybean GmFRF genes, 11 grape VvFRF genes, and 4 arabidopsis AtFRF genes that were screened were used to construct a phylogenetic tree (Figure 1). The results revealed that the FRF genes of the dicotyledonous plants such as soybean, arabidopsis, and grape were more closely related, whereas those of the monocotyledon grass crops barley and brachypodium were separated into a large branch. This indicated that the homology of FRF gene sequences between barley and brachypodium is higher than that of dicotyledonous plants.
Figure 1 Phylogenetic trees of FRF gene families in barley, brachypodium, soybean, grape, and arabidopsis. Multiple sequence alignments were performed with MEGA-11, and phylogenetic trees were constructed using the Neighbor-joining method. Light blue lines indicate the branch where the monocotyledonous plants (barley and brachypodium) FRF genes are located, and dark blue lines indicate the branch where the dicotyledonous plants (arabidopsis, soybean and grape) FRF genes are located. Blue triangles represent HvFRFs; green triangles represent BdFRFs; yellow squares represent GmFRFs; green squares represent VvFRFs, and red pentagrams represent AtFRFs.
3.3 Chromosomal localization and gene duplication events of HvFRF genes
The 22 HvFRF genes were unevenly distributed on the seven chromosomes of barley (Figure 2). The most densely distributed HvFRF genes were found on chromosomes 5H and 7H (7 and 5, respectively). The numbers of HvFRF genes on chromosomes 4H, 6H, 2H, and 3H were 4, 3, 2, and 1, respectively, whereas no HvFRF gene was found on chromosome 1H.
Figure 2 Chromosome localization of HvFRFs. The left bar indicates the length and physical position of the chromosome. The color of the bands on the chromosome represents gene density, where red and blue indicate regions of high and low gene densities, respectively.
To further analyze the evolutionary relationship of FRF genes in barley, the repeated events of 22 HvFRF genes in barley were analyzed. The results revealed no collinearity gene pair among the 22 HvFRF genes in barley, indicating that no gene duplication event occurred in the HvFRF gene family (Supplementary Figure S1).
3.4 Conserved motifs and gene structures of HvFRFs
To understand the sequence characteristics of the 22 HvFRF genes in barley, the conserved motifs (Figures 3B, E), core domains (Figure 3C), and gene structure characteristics (Figure 3D) were analyzed based on the evolutionary analysis (Figure 3A). The core domain analysis results revealed that all HvFRFs had one FAR1 domain (Figure 3C). The results of conserved motif analysis revealed that the HvFRF proteins of the same subfamily had similar motif composition (Figure 3B). Among them, 12 members of 13 HvFRF proteins of subfamily I contained conserved Motif 4, and each of the nine HvFRF proteins of subfamily II contained a long and conserved Motif 1. Subfamily II contained Motif 2, Motif 3, and Motif 5, accounting for 89%, 89%, and 67% of the members, respectively. The members of subfamily I contained Motif 2, Motif 3, and Motif 5, accounting for only 38%, 54%, and 15%, respectively. The members of subfamily II contained more than three different motifs accounting for 89%, whereas the members of subfamily I only accounted for 31%. It can be seen that compared with HvFRFs in subfamily I, subfamily II members had more types and numbers of Motifs, and the Motif composition was more regular. Gene structure analysis revealed that more than half of the HvFRF genes from subfamily I contained 1–3 introns; however, only 2 members of the 9 HvFRF genes from subfamily II contained one intron, and the remaining members had no introns (Figure 3D). These results suggested that the HvFRFs of subfamily II have a simpler gene structure.
Figure 3 Sequence characteristics of HvFRF genes. (A) Phylogenetic tree of HvFRF gene family; (B) Conserved motifs in HvFRF proteins; (C) Core domain of HvFRF proteins; (D) HvFRF gene structure; (E) Logo diagram of the five conserved motifs of HvFRF proteins.
3.5 Cis-element in the promoter of HvFRFs, transcription factor-HvFRF and miRNA-HvFRF regulatory networks
To understand the role of HvFRFs in stress response and signal transduction pathways in barley, the cis-elements in the 2000-bp promoter zone upstream of ATG of 22 HvFRF genes were analyzed using the PlantCARE website. The results revealed that the promoter zone of HvFRF genes contained a series of important hormone- and abiotic-stress-response elements, including ABRE, ARE, GARE, MBS, MRE, TCA-element, TGA-element, and MeJA-element (Figure 4) involved in ABA response, anaerobic induction regulation, gibberellin response, drought response, light response, salicylic acid response, auxin response, and methyl jasmonate response, respectively. Importantly, the composition and distribution of cis-elements in the promoter zone of HvFRF genes were clearly different between the two subfamilies. HvFRFs from subfamily I contained a large number of ABA and methyl jasmonate response elements; however, most HvFRFs from subfamily II contained gibberellin and salicylic acid response elements, and the distribution characteristics of the elements were similar. Additionally, except for HvFRF4, HvFRF6, HvFRF10, and HvFRF17, the promoter zones of other HvFRF genes contained essential element MBS in response to drought stress. HvFRF2, HvFRF9, and HvFRF14 genes from subfamily II simultaneously contained gibberellin, salicylic acid, and drought response elements.
Figure 4 Cis-element in the promoter of HvFRFs. (A) Phylogenetic tree of HvFRF gene family. (B) Schematic of cis-element in the promoter of HvFRFs.
To understand the regulation networks of transcription factors on HvFRFs, The upstream transcription factors of HvFRF genes were predicted. 4181 binding sites of 33 kinds of transcription factors are identified within the promoter regions of 22 HvFRF genes, among which, ERF and C2H2 are the two main types, with a binding site of 955 and 444, respectively (Supplementary Table S2). To determine whether a miRNA-HvFRFs regulatory network exists in barley, 71 known miRNAs were scanned. Finally, 3 miRNAs (hvu-miR5052, hvu-miR6199 and hvu-miR6200) were predicted to inhibit the transcription level of HvFRFs (HvFRF16, HvFRF8 and HvFRF10) (Supplementary Table S3).
3.6 Tissue expression characteristics and expression patterns of HvFRF genes in response to drought stress
To understand the expression of HvFRF genes in various developmental stages and various tissues of barley, the expression data of Morex varieties were downloaded from WheatOmics 1.0 and a heat map was plotted (Figure 5). The results revealed that the expression levels of HvFRF genes were significantly different in the root, epidermal cells, leaves, inflorescence, and grain at various developmental stages. Most HvFRF genes were expressed at low levels or even not expressed in all tissues. HvFRF9 gene was highly expressed in various tissues, particularly in the root, epidermis, rachis, palea, and developing grain.
Figure 5 Heat map of tissue expression of HvFRF genes. The larger the circle and redder the color, the higher the expression. PA, post-anthesis; DPA, day post-anthesis.
Abiotic stress is an important adverse factor that limits crop growth and grain yield, and drought is one of the main factors. To further study the expression characteristics of HvFRF genes under drought resistance, an analysis was conducted on the expression in response to drought stress of HvFRF9 with tissue expression advantages, as well as HvFRF1, HvFRF2, HvFRF14, and HvFRF22 genes in the same evolutionary branch as HvFRF9. The results revealed that all five genes were upregulated in PEG-treated roots of Golden promise barley in response to drought stress. Except for HvFRF2 gene, the expression levels of the other four genes reached the maximum at 3 h of drought treatment; however, HvFRF9 gene was the most significantly upregulated (3.9 times higher than the control) (Figure 6). With the extension of PEG-treatment time, the expression level of the five genes decreased and returned to that of the control at 24 h of treatment (Figure 6). According to the above results, HvFRF9 was upregulated most significantly in response to drought stress, and it was speculated that HvFRF9 was closely related to drought resistance in barley.
Figure 6 Expression patterns of HvFRF1, HvFRF2, HvFRF9, HvFRF14, and HvFRF22 in response to drought stress.
3.7 Cloning and expression localization of HvFRF9 in barley
The ORF of HvFRF9 gene was amplified using the DNA and cDNA from Golden promise roots as templates, and agarose gel electrophoresis revealed that the amplified products of DNA and cDNA were of the same size (Supplementary Figure S2A). The amplified products were ligated into the pEASY-Blunt vector and sequenced. The results revealed that the 789-bp ORF of HvFRF9 was intron-free and encoded a 262-aa protein sequence (Supplementary Figure S2B). Alignment of HvFRF9 protein sequence with arabidopsis AtFRF1, AtFRF2, AtFRFR3, and AtFRF4 protein sequences revealed that the above proteins contained a FAR1 conserved domain (Supplementary Figure S3A). The highly conserved amino acid residues among the five proteins were consistent with the HMM logo map of the FAR1 domain in the PFAM website (Supplementary Figure S3B). Secondary structure (Supplementary Figure S4A) and 3D (Supplementary Figure S4B) model prediction revealed that there were 7 helix and 9 strand in HvFRF9 protein sequence.
In-situ PCR was performed using the roots and leaves of Golden promise at the two-leaves and one-heart stage under hydroponic condition, and the staining of tissue sections was observed under a positive fluorescence microscope (DM6B, Leica, Wetzlar, Germany). In the roots, HvFRF9 transcripts were mainly detected in the phloem, xylem, and epidermal cells (Figure 7A); in the leaves, they were mainly detected in the phloem, xylem, and bundle sheath (Figure 7B). Therefore, HvFRF9 may be related to the absorption and transport of water and mineral nutrients in barley.
Figure 7 Localization of HvFRF9. Tissue sections of the HvFRF9 gene in barley roots and leaves under in-situ PCR are shown in (A, B), respectively. The 18S RNA amplification product was used as a positive control, and the sample without primers was used as a negative control. The two images on the far right are magnified images of the area in the red box. e, epidermis; c, cortical parenchyma cells; x, xylem; p, phloem, en, endodermis; bs, bundle sheath; ms, mesophyll. Bar = 100 μm. (C, D) indicate the subcellular localization of HvFRF9 in arabidopsis protoplasts and tobacco epidermal cells, respectively. GFP: green fluorescence channel, YFP: yellow fluorescence channel, NLS-mCherry: nuclear localization marker, Chlorophyll: chloroplast autofluorescence, Bright: light field, Merge: superposition of fluorescence and light field.
The subcellular localization vector of HvFRF9 was used to transform arabidopsis protoplasts and four-leaf tobacco using PEG and Agrobacterium-mediated methods, respectively. The subcellular localization of HvFRF9 was observed under a laser confocal microscope (A1 HD25, Nikon, Tokyo, Japan). The results revealed that HvFRF9 was localized only in the nucleus of arabidopsis protoplasts (Figure 7C). In tobacco epidermal cells, the gene was mainly located in the nucleus, and a small amount was also expressed in the chloroplast (Figure 7D). It can be concluded that HvFRF9 mainly functions in the nucleus and is a transcription factor.
3.8 Determination of the role of HvFRF9 in drought resistance via its overexpression in arabidopsis
To investigate the effects of drought stress on the root growth of HvFRF9-overexpressed and wild-type arabidopsis, arabidopsis seedlings were treated with 0, 50, 100, or 200 mM mannitol. No significant difference in root length and fresh weight was observed between wild-type and transgenic arabidopsis grown in MS medium without mannitol. Treatment with 50 mM mannitol slightly promoted the root length of wild-type and transgenic arabidopsis but inhibited the increase in the fresh weight of wild-type plants. With the increase of mannitol concentration, the inhibition of root growth of arabidopsis gradually increased; however, the degree of inhibition was significantly less in transgenic arabidopsis than in wild-type arabidopsis (Figure 8). The most obvious difference between the wild-type and transgenic lines was observed under the treatment of 200 mM mannitol; transgenic arabidopsis plants exhibited almost no wilting and yellowing of leaves, longer root systems, and more lateral roots than the wild-type plants (Figure 8A). Specifically, the average fresh weight of transgenic lines OE1, OE2, and OE3 was 0.0237, 0.0208, and 0.0188 g, respectively, whereas that of wild-type plants was only 0.0135 g. The fresh weight of transgenic lines was significantly higher than that of wild-type plants (Figure 8B). Moreover, the average root length of transgenic lines OE1, OE2, and OE3 (7.24, 7.07, and 6.27 cm, respectively) was significantly higher than that of wild-type plants (5.15 cm) (Figure 8C). These results indicated that HvFRF9 overexpression lines exhibited better resistance to drought stress under mannitol treatment than wild-type arabidopsis.
Figure 8 Effects of treatment with various concentrations of mannitol on HvFRF9-overexpressed and wild-type arabidopsis. (A) Growth phenotypes, (B) fresh weight, and (C) primary root length of HvFRF9-overexpressed and wild-type plants under various mannitol concentrations. Data are the means of three biological replicates. The different lowercase letters represent significant differences at the 5% level.
To further verify the role of HvFRF9 in drought resistance, a pot experiment was conducted to observe the phenotypes of HvFRF9-overexpressed and wild-type arabidopsis in response to drought stress, and the related physiological parameters were measured. No significant difference in terms of shoot growth was observed between HvFRF9-overexpressed and wild-type arabidopsis under normal watering condition. Under drought treatment, the growth of both overexpressed and wild-type plants was inhibited to a certain extent; however, the leaves of wild-type plants were severely wilted, turned yellow, and even fell off, whereas the HvFRF9 overexpression lines could still grow normally (Figure 9A). This indicated that in the HvFRF9 overexpression lines, growth was significantly less inhibited than in the wild-type plants under drought conditions. Additionally, drought treatment promoted the accumulation of O2− in the leaves compared with the normally watered plants; however, the accumulation of O2− was significantly lower in the leaves of the HvFRF9 overexpression lines than in those of the wild-type plants (Figure 9B). Under normal watering conditions, no significant difference was observed in terms of MDA content in the leaves between HvFRF9-overexpressed and wild-type arabidopsis. Drought treatment increased the MDA content; however, the increase in MDA in the leaves of HvFRF9 overexpression lines was significantly smaller than that in the leaves of wild-type plants (Figure 9C). Additionally, drought treatment increased CAT activity (Figure 9D), PRO content (Figure 9E), POD activity (Figure 9F), and SOD activity (Figure 9G) in the leaves compared with normal watering. However, CAT activity (Figure 9D), PRO content (Figure 9E), POD activity (Figure 9F), and SOD activity (Figure 9G) in the leaves of HvFRF9 overexpression lines were significantly higher than those in the leaves of wild-type plants. These results suggested that HvFRF9 overexpression could enhance the drought resistance of transgenic arabidopsis by increasing the antioxidant enzyme activity and reducing the increase in O2− and MDA contents.
Figure 9 The phenotypes and various physiological indices in response to drought stress in HvFRF9-overexpressed and wild-type arabidopsis were determined. (A) Growth phenotype, (B) O2− accumulation, (C) MDA content, (D) CAT activity, (E) PRO content, (F) POD activity, and (G) SOD activity in HvFRF9-overexpressed and wild-type arabidopsis under normal watering and drought treatment conditions. Data are the means of three biological replicates. The different lowercase letters represent significant differences at the 5% level.
4 Discussion
Drought is one of the important abiotic stress factors limiting crop growth and yield. Improving the drought-resistant ability of crops is of great significance. Exploring the drought-resistant genes and their function and mechanism is an important basis for developing new drought-resistant crops. Barley exhibits great adaptation and strong stress resistance characteristics. Therefore, it is an excellent material for exploring drought-resistance-related genes. FRS and FRF gene families are novel transcription factors derived from transposases, which play important roles in various life processes in plants such as light signal response, growth response, and stress response by regulating the expression of downstream genes (Ma et al., 2016). However, current studies on these genes are mainly focused on the model plant arabidopsis. To explore the evolution and function of FRF gene family in barley, 22 FRF genes in barley were identified from genome-wide analysis (Table 1), and HvFRF9 was identified to have drought resistance function. The discovery of this gene can provide a new gene resource for genetic improvement of drought resistance in plants.
4.1 FRS and FRF gene families involved in the regulation of drought resistance and other environmental adaptability in plants
Medicago ruthenica (L.) Trautv. is a wild perennial legume forage widely distributed in semiarid grasslands with outstanding tolerance to environmental stresses (Yoder et al., 2013). Genome sequencing and genetic studies have reported that the expansion of the FHY3/FAR1 family in the wild M. ruthenica played an important role in drought stress tolerance compared with the cultivated alfalfa (Wang et al., 2021). It has been demonstrated that FHY3/FAR1 in arabidopsis is a positive regulator of ABA signaling and can exhibit increased expression in response to ABA and abiotic stresses. Compared with the wild type, fhy3 and far1 mutants exhibit wider stomata and faster water loss and are more sensitive to drought (Li et al., 2016). Myo-Inositol-1-phosphate synthase (MIPS) is a rate-limiting enzyme that catalyzes the biosynthesis of inositol and plays a crucial role in plant growth and development. In arabidopsis, FHY3/FAR1 directly binds to the promoter of MIPS1 and activates its expression, thereby promoting inositol biosynthesis and preventing light-induced oxidative stress and SA-dependent cell death (Joly-Lopez et al., 2016). Abiotic stresses, particularly salt and temperature stresses, are important environmental factors affecting wood productivity. In Eucalyptus grandis W. Hill ex Maiden, FHY3/FAR1 family genes play a role in the response to salt and temperature treatments, and these genes may be used in improving wood yield of E. grandis (Dai et al., 2022). FHY3 can interact with MYC2, a key transcription regulator of jasmonic acid response, and coregulate the expression of jasmonic-acid-responsive defense genes (Liu et al., 2019). In Camellia sinensis (L.) O. Kuntze, most CsFHY3/FAR1s are upregulated in response to drought stress. Genetic and molecular evidence suggested that FRS7 and FRS12 interact with NOVEL INTERACTOR OF JAZ (NINJA) to regulate glucosinolate-biosynthesis-related genes and participate in the defense mechanism of arabidopsis (Fernández-Calvo et al., 2020). Expression analysis revealed that some HvFRF genes identified in this study were significantly upregulated in response to drought stress (Figure 6), suggesting that some of these members play a role in drought resistance in barley.
4.2 The FRF gene in barley is evolutionarily specific
During long-term evolution, genes derived from the same ancestor (that is, the sequences of different members of the same gene family) become different, and each gene exhibits different expression regulation patterns and plays different functions (Mitchell-Olds and Schmitt, 2006). The study of gene families can help in understanding the evolutionary history of a class of genes, in determining whether there is a specific gene family in a species, and in discovering important functional genes (Thornton and DeSalle, 2000). FRF family members have only one FAR1 domain, which is considered to be a truncated FRS protein. It can compete with FRS for the binding site of target genes and play a regulatory role on target genes (Ma et al., 2016). At present, research on the FRF genes in crops is still very limited. In this study, Blast and hummer search identified various numbers of FRF genes from the genomes of dicotyledonous plants (soybean and grape). However, except for barley and brachypodium, FRF family genes were not found in other monocotyledonous crops (wheat, maize, rice, and sorghum). This demonstrated that FRF family genes are unique to barley and brachypodium in these monocotyledonous crops, suggesting that FRF family genes have specific roles in growth and development or stress resistance in barley. Meanwhile, in terms of evolution, the FRF genes of monocotyledonous plants (barley and brachypodium) and dicotyledonous plants (arabidopsis, soybean and grape) are on completely different branches (Figure 1). This indicated that the FRF genes of monocotyledonous and dicotyledonous plants are distantly related, and the FRF family members of barley and brachypodium are relatively more specific in evolution. Studies have reported that the main causes of gene family expansion include genome polyploidy, tandem duplication, fragment duplication, retrotransposition or exon duplication, and reorganization (Zhu et al., 2014; Bai et al., 2022). However, no collinearity gene pair was observed among the 22 HvFRF genes identified in this study (Figure S1), indicating that each member of the HvFRF gene family is relatively independent and may have different functions.
4.3 The promoter zone of FRF genes in barley contains abundant adversity-stress-response elements
Promoters are gene switches located in the upstream of the coding region of genes, which turn on and off the functional activity of genes and contain specific cis-elements. These elements are the binding targets of upstream regulatory genes, and they regulate the expression of target genes by binding to upstream genes (Hernandez-Garcia and Finer, 2014; Villao-Uzho et al., 2023). The analysis of cis-elements in the promoter region of HvFRFs revealed that the promoter region of HvFRFs contains a large number of hormone- and abiotic-stress-response elements. Significant differences were observed in element types and distribution characteristics between members of subfamilies I and II (Figure 4), indicating that HvFRF genes from subfamilies I and II may play different functions. The results revealed that MaTIP1;2 gene promoter contains salicylic-acid-response element (TCA-element), which was introduced into A. thaliana to enhance drought and salt stress resistance (Song et al., 2018). Since various stresses can induce ABA synthesis, ABA is considered as a plant stress hormone (Yoon et al., 2020). Many genes that respond to ABA signals contain ABRE elements in the promoter zones, and these genes often play a role in the response of plants to abiotic stress (Dinneny et al., 2008). For example, the DREB2A gene in arabidopsis has the function of drought resistance (Kim et al., 2011), and the OsDREB gene in rice responds to drought, high-salt, and low-temperature stresses (Dubouzet et al., 2003). The promoter zones of drought- and salt-tolerance genes in arabidopsis contain a certain amount of TCA-element, ABRE, gibatellin-responsive element (GARE motif), methyl jasmonate response element (MeJA-element), and drought-response element (MBS) (Shariatipour and Heidari, 2018). In this study, the promoter zone of HvFRF genes in subfamily I contained a large amount of ABRE and MeJA-element, whereas that in subfamily II contained more TCA-element and GARE motifs. Additionally, the promoter region of some members contained MBS (Figure 4). Thus, it is speculated that HvFRF genes bind to upstream regulators through cis-elements in the promoter zone and play a role in abiotic stress resistance.
4.4 HvFRF9 plays an important role in drought resistance
The results of tissue expression profiling revealed that the expression of HvFRF9 in various tissues of barley was obviously higher than other HvFRFs (Figure 5). To identify the FRF genes related to drought resistance in barley, the expression characteristics of HvFRF genes in the same evolutionary branch as HvFRF9 in response to drought stress were analyzed. The results revealed that HvFRF9 gene responded most significantly to drought stress (Figure 6), suggesting that this gene was involved in the regulation of drought resistance in barley. The epidermal cells of the root are in direct contact with the soil and are the main parts that absorb water and nutrients. In addition, the epidermal cells can form root hair increasing the surface area of the root system, which is conducive to the absorption of water and nutrients (He et al., 2015). Compared with in-situ hybridization, in-situ PCR is a relatively simple and rapid method for detecting the location of gene expression (Athman et al., 2014). The results of in-situ PCR revealed that HvFRF9 was highly expressed in the epidermal cells of barley root (Figure 7A), indicating that this gene is beneficial for the absorption of water or nutrients by roots. Xylem and phloem are responsible for transporting water absorbed by roots and ions dissolved in water, making them available for other tissues or organs; additionally, they provide support to plant body (Huang et al., 2018). HvFRF9 was mainly expressed in the xylem and phloem of barley roots and leaves (Figure 7A), indicating that this gene also plays a role in water or nutrient transport.
Drought stress can decrease the relative water content in the leaves, resulting in leaf wilting and stem tip bending, which affects the normal growth of plants (Fang and Xiong, 2015). Meanwhile, drought stress can lead to excessive ROS accumulation in plants, causing oxidative damage to plants (Lee and Park, 2012). Additionally, MDA content in plants increased after drought stress, resulting in cytoplasmic membrane damage (Ma et al., 2015). In this study, under drought stress, the degree of loss of green color, wilting, O2− accumulation, and MDA content were lower in the leaves of HvFRF9-overexpressing arabidopsis than in those of wild-type plants (Figures 8, 9). This suggested that overexpression of HvFRF9 improved the ability of arabidopsis to resist drought. Osmotic regulation is an important mechanism for plants to resist drought stress. Plants can adapt to the external environment by regulating the osmotic potential of cells (Dubois and Inzé, 2020). PRO is an important osmoregulatory organic substance, and increase in its content under drought conditions helps to prevent cell or tissue dehydration (Wang et al., 2022). In the process of resisting stress, plants have evolved a complex antioxidant system to reduce the production of excessive ROS and avoid serious oxidative damage to plants. It mainly includes SOD, POD, CAT, and other antioxidant enzymes (Ahmadi et al., 2022). SOD, as the first line of antioxidant defense, converts O2− into H2O2 and O2 through the dismutation reaction, and CAT and POD further convert toxic endogenous H2O2 into H2O and O2 (Anjum et al., 2012). Under drought stress, the increase in PRO content and SOD, CAT, and POD activities were significantly higher in HvFRF9-overexpressing arabidopsis than in wild-type plants (Figure 9). These results indicated that HvFRF9 could reduce the osmotic stress and increase the antioxidant ability of the plants by increasing the PRO content and antioxidant enzyme activities, thus enhancing the drought resistance of the plants.
In conclusion, drought is one of the most dominant abiotic stresses affecting growth and yield of crops. FRF genes are novel transcription factors unique in plants. They play a role in stress resistance in plants. With wide adaptability and high stress-resistance, barley is an excellent candidate for the identification of stress resistance genes. However, studies on the FRF genes in barley are few. In this study, 22 HvFRFs were identified using genome-wide analysis, and their gene sequence, gene structure, evolutionary relationship, chromosome localization, cis-element in promoter, collinearity, tissue expression site, and expression profile in response to drought stress were analyzed. HvFRF9 with significantly upregulated expression in response to drought stress was identified. Under drought stress, leaf chlorosis and wilting and MDA and O2− contents were significantly lower and fresh weight; root length; PRO content; and SOD, CAT, and POD activities were significantly higher in HvFRF9-overexpressed arabidopsis than in wild-type plants. This suggested that HvFRF9 overexpression could enhance drought resistance in arabidopsis. Therefore, HvFRF9 exhibits drought resistance function. This study enhanced the understanding of drought resistance in plants and provided candidate genes for genetic improvement of drought resistance in barley or other plants.
Data availability statement
The original contributions presented in the study are included in the article/Supplementary Material. Further inquiries can be directed to the corresponding author.
Author contributions
XH: Conceptualization, Data curation, Funding acquisition, Investigation, Supervision, Visualization, Writing – original draft, Writing – review & editing. YH: Data curation, Formal analysis, Supervision, Writing – review & editing. YD: Conceptualization, Data curation, Formal analysis, Investigation, Writing – original draft. YG: Data curation, Writing – original draft. XS: Data curation, Writing – original draft. WC: Data curation, Validation, Writing – original draft. XX: Validation, Writing – original draft. CS: Validation, Writing – original draft. YL: Validation, Writing – original draft. BR: Validation, Writing – original draft. HY: Validation, Writing – original draft. JZ: Funding acquisition, Supervision, Writing – review & editing. WM: Supervision, Writing – review & editing. PM: Conceptualization, Funding acquisition, Supervision, Writing – review & editing.
Funding
The author(s) declare financial support was received for the research, authorship, and/or publication of this article. This work was supported by the Natural Science Foundation of Shandong Province (ZR2021MC025), the National Natural Science Foundation of China (32171976), the Wheat Innovation Team of Modern Agricultural Production Systems in Shandong Province (SDAIT01-05) and the High-Level Talents Project of Qingdao Agricultural University (663/1119013).
Acknowledgments
The authors would like to thank all the reviewers who participated in the review.
Conflict of interest
The authors declare that the research was conducted in the absence of any commercial or financial relationships that could be construed as a potential conflict of interest.
Publisher’s note
All claims expressed in this article are solely those of the authors and do not necessarily represent those of their affiliated organizations, or those of the publisher, the editors and the reviewers. Any product that may be evaluated in this article, or claim that may be made by its manufacturer, is not guaranteed or endorsed by the publisher.
Supplementary material
The Supplementary Material for this article can be found online at: https://www.frontiersin.org/articles/10.3389/fpls.2024.1347842/full#supplementary-material
Supplementary Figure 1 | Gene duplication events in HvFRFs in barley. From outside to inside are the schematic diagram of the seven chromosomes in barley, peak map of gene density on barley chromosomes, and scale of gene density on barley chromosome, with red and blue representing the regions of high and low gene densities, respectively.
Supplementary Figure 2 | Cloning results of HvFRF9. (A) Agarose gel electrophoresis of HvFRF9 cDNA and DNA. (B) Nucleotide and amino acid sequences of the ORF region of HvFRF9. M: DL2000 DNA marker; 1: cDNA amplification bands of HvFRF9; 2: DNA amplification bands of HvFRF9.
Supplementary Figure 3 | Amino acid sequence alignment analysis of HvFRF9 with four FRF in arabidopsis. (A) Amino acid sequences; the part marked in red is the FAR1 conserved domain. (B) HMM logo plot of the conserved domain of FAR1, with larger letters indicating more conserved amino acids.
Supplementary Figure 4 | Structural prediction of HvFRF9 gene. (A) The secondary structure of HvFRF9. (B) The 3D model of HvFRF9.
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Keywords: drought stress, barley (Hordeum vulgare L.), HvFRFs gene family, HvFRF9, functional identification
Citation: He X, He Y, Dong Y, Gao Y, Sun X, Chen W, Xu X, Su C, Lv Y, Ren B, Yin H, Zeng J, Ma W and Mu P (2024) Genome-wide analysis of FRF gene family and functional identification of HvFRF9 under drought stress in barley. Front. Plant Sci. 15:1347842. doi: 10.3389/fpls.2024.1347842
Received: 01 December 2023; Accepted: 09 January 2024;
Published: 24 January 2024.
Edited by:
Weiqiang Li, Chinese Academy of Sciences (CAS), ChinaReviewed by:
Sumaira Rasul, Bahauddin Zakariya University, PakistanAnuj Kumar, Dalhousie University, Canada
Copyright © 2024 He, He, Dong, Gao, Sun, Chen, Xu, Su, Lv, Ren, Yin, Zeng, Ma and Mu. This is an open-access article distributed under the terms of the Creative Commons Attribution License (CC BY). The use, distribution or reproduction in other forums is permitted, provided the original author(s) and the copyright owner(s) are credited and that the original publication in this journal is cited, in accordance with accepted academic practice. No use, distribution or reproduction is permitted which does not comply with these terms.
*Correspondence: Ping Mu, muping@qau.edu.cn
†These authors have contributed equally to this work