Next Article in Journal
Evaluation of the Maturity and Gene Expression of Sheep Oocytes and Embryos Cultured in Media Supplemented with Marjoram (Origanum vulgare) Extract
Previous Article in Journal
FBN1 Splice-Altering Mutations in Marfan Syndrome: A Case Report and Literature Review
 
 
Search for Articles:
Title / Keyword
Author / Affiliation / Email
Journal
Article Type
 
 
Advanced Search
 
Section
Special Issue
Volume
Issue
Number
Page
 
Journals
Genes
Volume 13
Issue 10
10.3390/genes13101843
genes-logo
Submit to this Journal Review for this Journal Propose a Special Issue
► Article Menu

Article Menu

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

Function and Evolution of C1-2i Subclass of C2H2-Type Zinc Finger Transcription Factors in POPLAR

by
Ping Li
,
Anmin Yu
,
Rui Sun
and
Aizhong Liu
*
Key Laboratory for Forest Resource Conservation and Utilization in the Southwest Mountains of China (Ministry of Education), Southwest Forestry University, Kunming 650224, China
*
Author to whom correspondence should be addressed.
Genes 2022, 13(10), 1843; https://doi.org/10.3390/genes13101843
Submission received: 2 September 2022 / Revised: 24 September 2022 / Accepted: 11 October 2022 / Published: 12 October 2022
(This article belongs to the Section Plant Genetics and Genomics)
Browse Figures
Review Reports Versions Notes

Abstract

:
C2H2 zinc finger (C2H2-ZF) transcription factors participate in various aspects of normal plant growth regulation and stress responses. C1-2i C2H2-ZFs are a special subclass of conserved proteins that contain two ZnF-C2H2 domains. Some C1-2i C2H2-ZFs in Arabidopsis (ZAT) are involved in stress resistance and other functions. However, there is limited information on C1-2i C2H2-ZFs in Populus trichocarpa (PtriZATs). To analyze the function and evolution of C1-2i C2H2-ZFs, eleven PtriZATs were identified in P. trichocarpa, which can be classified into two subgroups. The protein structure, conserved ZnF-C2H2 domains and QALGGH motifs, showed high conservation during the evolution of PtriZATs in P. trichocarpa. The spacing between two ZnF-C2H2 domains, chromosomal locations and cis-elements implied the original proteins and function of PtriZATs. Furthermore, the gene expression of different tissues and stress treatment showed the functional differentiation of PtriZATs subgroups and their stress response function. The analysis of C1-2i C2H2-ZFs in different Populus species and plants implied their evolution and differentiation, especially in terms of stress resistance. Cis-elements and expression pattern analysis of interaction proteins implied the function of PtriZATs through binding with stress-related genes, which are involved in gene regulation by via epigenetic modification through histone regulation, DNA methylation, ubiquitination, etc. Our results for the origin and evolution of PtriZATs will contribute to understanding the functional differentiation of C1-2i C2H2-ZFs in P. trichocarpa. The interaction and expression results will lay a foundation for the further functional investigation of their roles and biological processes in Populus.

1. Introduction

Zinc-binding domains were first identified in the protein TFIIIA of Xenopus oocytes, and function in the binding of IIA and DNA with cysteines and histidines in the enrichment folding domain centered on a zinc ion [1]. Zinc finger proteins (ZnFs) are the abundant proteins in eukaryotes, with diverse functions, including DNA recognition, RNA packaging, transcription regulation, protein folding, and assembly [2]. Structure studies of ZnFs revealed their diversity, which can be classified into classical, GATA, RanBP and A20 ZnFs according to their zinc ligation topology [3]. Classical ZnFs include a short β hairpin and α helix with a zinc atom coordinated with Cys-Cys-His-His or Cys-Cys-His-Cys subunits [3]. Most classical ZnF Cys2His2 zinc fingers are transcription factors that provide DNA binding and transcription regulation via their ββα framework of a Cys2His2 (C2H2) zinc finger module [2]. The stability of the C2H2 zinc finger ββα framework is maintained by the interlaced linkage provided by Zn2+, which binds with two pairs of histidines at the C-terminus of the α-helix and two cysteines at the end of the β-strand [4]. RS_CRZ1, a C2H2 ZnF of the tomato plant, is involved in the hostile environment encountered during Rhizoctonia solani host colonization [5].
The function of C2H2 ZnFs in growth regulation has been reported in plants. POPOVICH (POP), which encodes a C2H2 zinc-finger transcription factor (C2H2 ZTF), plays an important function during the evolution of Aquilegia nectar by regulating cell proliferation during the early phase of spur development [6]. VviZEPs may be a candidate regulator of pollen and grapevine reproductive development [7]. Hair, which encodes C2H2 ZnF, regulates trichome formation in Solanaceae species, where knockout and overexpression can directly repress or trigger trichome formation [8]. C2H2 ZTF encodes SE3.1, which is involved in the transition process from stigmas exsertion to insertion and affects the rate of self-fertilization in tomatoes [9]. Non Stop Glumes1 (NSG), encodes C2H2 ZTF, which can bind to Leafy Hull Sterile1 (LHS1) and recruits the corepressor TOPLESS-related protein to repress expression by downregulating histone acetylation levels of the chromatin, and then maintains an organ identified in the spikelet of Oryza sativa [10].
Stress resistance is another recognized function that involves C2H2. TaZFP1B, a C2H2-ZEP type transcription factor gene of wheat, can regulate P acquisition, ROS homeostasis and root system establishment to enhance plants’ Pi deprivation tolerance [11]. Overexpression of TaZFP1B can stimulate plant growth and oxidative resistance, which enhances wheat drought tolerance at critical periods [12]. PeSTZ1, a C2H2 ZTF coding gene of Populus euphratica, directly regulates PeAPX2 (ascorbate peroxidase of P. euphratica) to modulate plant ROS scavenging and enhances the freezing tolerance of poplar [13]. GhSTOP1, a C2H2 ZTF of Gossypium hirsutum L., can impact GhALMT1 (Aluminum-activated Malate Transporter 1), GhMATE (Multidrug and Toxic Compound Extrusion) and GhALS3 (Aluminum Sensitive 3) to regulate aluminum and proton stress tolerance of cotton [14]. MpZEF1, a C2H2 ZTF of Millettia pinnata, can increase the accumulation of stress-responsive genes and reduce reactive oxygen species (ROS) to enhance plant salt stress resistance [15]. Except for the influence on stress responses, C2H2 ZTFs may regulate the catechin accumulation of Camellia sinensis (L.) O. Kuntze [16].
Based on the protein pattern, all the C2H2 ZTFs of Arabidopsis thaliana were divided into three sets (A, B and C), and each set was further divided into different families as C1, C2 and C3 in set C [17,18]. Family C1 comprised conserved zinc finger helices with an invariant QALGGH motif, which can be subdivided into C1-1i, C1-2i, C1-3i, C1-4i, and C1-5i according to the number of isolated fingers [18]. The 20 C1-2i members of A.thaliana were assigned into five subgroups (C1-2iA, C1-2iB, C1-2iC, C1-2iD, and C1-2iX) according to sequence similarity [18]. ZATs (Zn transporter of A. thaliana) were a subtype of C1-2i Classical ZnFs Cys2His2 zinc fingers, whose function was unclear [18]. The four ZATs of the C1-2iD subgroup were involved in water stress response and salt resistance, which can be speculated from their expression change [19]. Van et al. isolated ZAT genes and found its 398 amino acid residues predicted six membrane-spanning domains in transgenic plants that can enhance Zn resistance and maintain Zn homeostasis [20]. GmZAT4, a typical C2H2 ZTF of soybean, can enhance plant osmotic and salt stress resistance and ABA responses through overexpression [21]. MdZAT10, a C2H2 ZTF gene of the‘Royal Gala’ apple and a homolog of Arabidopsis ZAT10, was negatively regulated for the drought tolerance of the apple by inducing a higher malondialdehyde (MDA) content and higher reactive oxygen species (ROS) [22]. ZATs can be affected by DNA methylation, whose methylation level was significantly greater in adult leaves than juvenile leaves, which limited their function in the mature period in Malus hupehensis [23]. Seven ZATs were discovered in M. hupehensis [23].
Although many studies have found important functions of C2H2 ZTF, a comprehensive investigation of ZATs (C1-2i C2H2-type zinc finger transcription factors), which are an important subtype of C2H2 ZTF, has not yet been completed. In the present study, we will investigate the structure and predict the function of ZATs in P. trichocarpa and different P. species. We first identified eleven PtriZATs in P. trichocarpa. The phylogenetic relationship, two conserved ZnF-C2H2 domains, motifs, gene structure, and cis-elements were characterized. The expression pattern of PtriZATs in different growth stages and stress resistance were analyzed. The distribution and structure of ZATs in different Populus species were also analyzed. Accordingly, our results provide information for ZATs in Pupulus and suggestions for further function investigation.

2. Materials and Methods

2.1. Identification of PtriZAT Members in P. trichocarpa and Populus Speciecs

To identify members of ZAT in P. trichocarpa, a sequence similarity search was performed using the Arabidopsis ZAT proteins with BLASTP of the standalone BLAST+ tool (NCBI-blast-2.7.1+) [18]. Seventeen proteins were obtained with similarity to A. thaliana ZATs (E-value ≤ 0.05). Protein sequences of identified ZAT homologs in P. trichocarpa were subjected to domain analysis using PFAM (https://pfam.xfam.org/ (accessed on 19 January 2022)), SMART (http://smart.embl-heidelberg.de/ (accessed on 27 January 2022)) and Web CD-Search Tool (https://www.ncbi.nlm.nih.gov/Structure/bwrpsb/bwrpsb.cgi (accessed on 17 January 2022)). According to the structure of ZAT domains, eleven proteins were analyzed as ZATs in P. trichocarpa. ZATs in different Populus were obtained by BLASTP with protein sequences of PtriZATs. The genome data of Populus deltoids, P. euphratica, Populus alba and Ptomentosa tomentosa were acquired from NCBI (https://www.ncbi.nlm.nih.gov/ (accessed on 24 January 2022)). The subcellular localization of PtriZATs was predicted by WOLF PSORT (https://wolfpsort.hgc.jp/ (accessed on 24 January 2022)). The features of proteins were analyzed using Expasy-ProtParam (https://web.expasy.org/protparam/ (accessed on 26 January 2022)).

2.2. Phylogenetic Relationship of ZAT Proteins in P. trichocarpa

The sequences of 11 ZAT proteins in P. trichocarpa were obtained from Phytozome13 (https://phytozome-next.jgi.doe.gov/ (accessed on 20 January 2022)). To analyze the phylogenetic relationship between different ZATs in P. trichocarpa, their full-length protein sequences were aligned using ClustalW [24]. The phylogenetic tree of ZAT proteins was constructed using MEGA11 with the Maximum Likelihood (ML) method [25]. The bootstrap values reported for each branch reflected the percentage of 1000 replicate trees containing that branch.

2.3. Exon Intron Structure, Location, Conserved Motifs and Promoter in PtriZAT Genes

The exon intron structures of eleven PtriZAT genes were analyzed using the Gene Structure View package of TBtools (v1.098691) with geneID and gff3 data of P. trichocarpa [26]. The chromosomal location of all identified PtriZAT genes on the chromosome was mapped using Chromosome Map Tool Blast, Text merge for MCScanx, Quick run MCScanX Wrapper and circle gene view packages of TBtools (v1.098691). The conserved motifs in PtriZAT proteins were searched using Multiple Em for Motif Elicitation (MEME) (https://meme-suite.org/meme/tools/meme (accessed on 19 January 2022)). The conserved cis-elements in the promoters of PtriZAT genes were analyzed using the PLACE database (https://www.dna.arc.go.jp/PLACE/ (accessed on 19 January 2022)) with the 2 kb sequences upstream of the translational start codon.

2.4. Plant Materials and qRT-PCR Assays

The poplars were gathered from Kunming (E102.74°, N25.17°), and well grown in the culture room of Southwest Forestry University, Kunming, with the cutting method and natural culture conditions. The fresh and healthy leaves, stems, and roots were collected. For drought, ABA, and salt treatment, there was a no-watering protocol (seven days), and 10 μM ABA and 250 Mm NaCl were added into the normal condition. Total RNAs were extracted using the RNAprep Pure Plant Plus Kit (Cat. DP441, Tiangen, Beijing, China) following the manufacturer’s instructions for different tissues and stress treatment plant materials. RNA (1 μg) was used for reverse transcription with an EasyScript® All-in-One First-Strand cDNA Synthesis SuperMix for qPCR reagent Kit (Transgene, Beijing, China). The relative expression levels of individual genes were measured with gene-specific primers (Table S1) by real-time quantitative PCR (qRT-PCR) analysis, which was carried out in a 20 μL reaction mix with 1 μL of diluted cDNA template and TransStart® Green qPCR SuperMix (Transgene, Beijing, China) with a Bio-Rad CFX96. The elongation factor 1 (EF1) served as the internal control [27].

2.5. Expression Profiles of PtriZAT Genes in Different Plants

P. trichocarpa and Physcomitrium patens transcriptome data were obtained from Phytozome 13 (https://phytozome-next.jgi.doe.gov/ (accessed on 20 January 2022)). The expression data of PtriZAT genes were used to analyze the expression profile of P. trichocarpa H1 genes at different development stages (female, male, bud, leaf, root, and stem) and treatments (ABA, ACC, BAP, BL, GA, NAA, SA, SL, and meJA). All the expression values demonstrated in the heatmap were calculated with log2 of the FPKM values of Phytozome 13. The heatmap of PtriZAT genes was obtained by Heml 1.0.3 [28].

2.6. Prediction of the Interaction Proteins of PtriZATs

The potential interaction proteins of PtriZATs were predicted using an online STRING server (https://string-db.org (accessed on 17 March 2022)) with the protein sequences of PtriZATs. All the interaction proteins of different PtriZATs were examined using contrastive analysis; the number and messages of corresponding proteins are listed in Table S2. The function annotation of interaction proteins was obtained in Phytozome 13.

3. Results

3.1. Genome-Wide Identification of PtriZAT Members in P. trichocarpa

After a sequence similarity search in P. trichocarpa with the 20 C1-2i C2H2 ZTF members of A. thaliana, 17 proteins of P. trichocarpa were obtained (Table S3). Of the 17 candidate proteins, only 11 members that were conserved contained two ZnF_C2H2 domains, which was the specific feature of C1-2i subclass ZFs (Table 1, Figure 1A [18]). The subcellular localization of 11 PtriZATs proteins predicted by WOLF PSORT showed their nucleus location (https://wolfpsort.hgc.jp/ (accessed on 24 January 2022)). The length of PtriZATs proteins varied from 179 to 310 amino acids. The length of Zn-C2H2 domains also varied from 24 to 26 amino acids. All the PtriZATs were neutral or basic proteins, which were aliphatic with low hydropathicity (Table 1).
To compare with other plants, we performed a homology search for typical plants using Arabidopsis ZATs through forward- and reverse-comparison, and confirmed the ZAT proteins with two Zn-C2H2 domains using the Web CD-Search Tool. Carya illinoinensis, Oryza sativa, Lactuca sativa, Manihot esculenta, Medicago truncatula, Solanum Tuberosum, and Zea mays contained more ZATs than P. trichocarpa. Ceratodon purpureus, β vulgaris L., Theobroma cacao, and Vitis vinifera had a small number of ZATs (Table S4).

3.2. Sequence Characteristics and Phylogenetic Relationships of PtriZATs

To obtain the sequence characteristic of PtriZATs, all 11 proteins were aligned and analyzed using BioEdit version 7.0.9.0 [29]. All the PtriZATs had two conserved ZnF-C2H2 domains with a specific plant QALGGH motif [18]. The 11 PtriZATs can be classified into 2 subgroups according to their sequence characteristics of the ZnF-C2H2 domain (Figure 1A). Seven PtriZATs (Potri.004G216900, Potri.006G121600, Potri.008G032300, Potri.010G229400, Potri.010G209400, Potri.001G235800, and Potri.009G027700) were conserved and had Lys134, Thr135, Arg150, and Lys154 during the first ZnF_C2H2 domain and Gly218, Glu220 (Val220 in Potri.008G032300), Met231, Arg233, and Arg235 during the second ZnF_C2H2 domain, which belonged to subgroup I. The other four PtriZATs (Potri.001G295500, Potri.009G089400, Potri.002G119300, and Potri.014G017300) replaced the conserved subunit with Thr/Ser134, Val135, Lys150, Arg154, His218, Thr220, Lys231, Cys233, and Tyr235, which belonged to subgroup II. The different subunits of PtriZATs did not influence the protein structure. All the PtriZATs contained two ZnF-C2H2 domains, which were ββα frameworks with a linkage interlaced by Zn2+ (Figure 1B,C).
According to the characteristic bases of C1-2i ZTFs of A. thaliana, PtriZATs belonged to the C1-2iC and C1-2iD subgroups [18]. The subgroup I PtriZATs were conserved and contained Arg138, Ser142, Phe143, Arg50, Lys54, and Arg/Lys55 in the helix of the first ZnF-C2H2 domain, and Gly224, Met231, Arg232, Arg233, and Arg235 in the helix of the second ZnF-C2H2 domain, which was characteristic of C1-2iC ZEPs of A. thaliana. The subgroup II PtriZATs substitute contained Lys138, Ser142, Tyr143, Lys50, Arg54, and Lys55 in the helix of the first ZnF-C2H2 domain, and Lys219, Thr223, Gly224, Lys231, Arg232, Cys233, and Tyr235 in the helix of the second ZnF-C2H2 domain, which was characteristic of C1-2iD ZEPs of A. thaliana (Figure 1A).
To understand the phylogenetic relationship of PtriZATs, a phylogenetic tree was built with sequences of PtriZAT proteins. The phylogenetic tree of PtriZATs revealed seven proteins that belonged to the same branches, consistent with the analysis results for protein structure (Figure 1 and Figure 2A). The other four PtriZATs belonged to the other branch with longer footsteps. To analyze the phylogenetic relationship of PtriZATs with subclass C1-2i ZEPs of A. thaliana, an unrooted tree was constructed with their protein sequences. Except for the C1-2iD subgroup ZEPs, the other A. thaliana ZEPs were separated into an independent branch (Figure S1). The phylogenetic tree of ZATs of a different plant also showed the two conserved subtypes of PtriZATs, which were sorted into two different branches with most ZATs of different plants, which may be according to different evolutionary relationships and sequence variation (Figure S2).

3.3. Gene, Protein Structure, and Conserved Motifs of PtriZAT Genes

To further understand the structure of PtriZATs, we searched 15 conserved motifs in PtriZATs with the MEME software. As shown in Figure 2B, motif1, motif2, and motif3 were the most conserved motifs, which were identified in all the PtriZATs. Subgroup II PtriZATs had seven conserved motifs (motif 1, motif 2, motif 3, motif 4, motif 5, motif 6, and motif 8). PtriZATs of subgroup I can be classified into two subtypes, Potri.004G216900, Potri.006G121600, Potri.008G032300, and Potri.010G229400 were the first subtype, which conservedhad motif1, motif2, motif3 and motif5. Potri.010G209400, Potri.001G235800 and Potri.009G027700 were the second subtype, which when conserved had motif 1, motif 2, motif 3, motif 4 and motif 7. The PtriZATs of subgroup II were conserved and had motif 1, motif 2, motif 3, motif 4, motif 5, motif 6 and motif 8 (Table S5). Protein structure analysis of PtriZATs found two conserved ZnF-C2H2 domains, the locations of which differed according to the subgroups (Figure 2C). The first subtype, PtriZATs of subgroup I, had longer sequences, with ZnF-C2H2 domains near the C-terminal. Meanwhile, the second subtype, PtriZATs of subgroup I, had the shortest sequences. To reveal the coding characteristic of PtriZATs, the gene structure was investigated by comparing the CDS sequences. The results showed that all PtriZAT genes were conserved and had a single exon, except for Potri.006G121600, which contained two exons linked with a short intron and without UTR sequences (Figure 2E).

3.4. Chromosomal Location and Duplication Events of PtriZAT Genes

To investigate the possible relationship between PtriZATs, we analyzed their chromosomal location using TBtools (Figure 3). We found eleven PtriZATs genes distributed on eight chromosomes randomly. No PtriZATs were located on chromosome 3, 5, 7, 11, 12, and 13. Except for Potri.001G235800, Potri.001G295500, Potri.009G027700, Potri.009G089400, Potri.010G229400, and Potri.010G209400, other PtriZATs were located on chromosome 2, 4, 6, 8, and 14 separately. Potri.008G032300, Potri.014G017300, Potri.004G216900, Potri.010G229400 and Potri.010G209400 were located on the distal ends of chromosomes 8, 14, and 10. The distribution of PtriZAT genes relative to the corresponding duplication is shown in Figure 3B. Potri.008G032300 was probably the primordial PtriZAT, which replicated to Potri.004G216900, Potri.006G121600, and Potri.010G229400 with genome duplication [30]. The other PtriZATs with synteny contained conserved ZnF-C2H2 domains and belonged to the same subgroup, which probably developed because of genome duplication [30].

3.5. Cis-Elements in the Promoter Regions of PtriZAT Genes

To investigate the regulation pattern, we detected cis-elements in the promoter regions of PtriZAT genes (Figure 2D, Table S6). Many cis-elements related to stress response and growth regulation were predicted by PlantCARE. The most frequent cis-elements were G-Box, which were detected in ten PtriZATs, except Potri.001G235800, which suggested the important function of light signals during transcription regulation. ABRE was the other widespread cis-elements in PtriZATs, which participated in the response of abscisic acid (ABA), which indicates the function of PtriZATs during stress response and growth regulation. The TGACG-motif, TC-rich repeats, LTR, AACA_motif, P-box, MBS, TCA-element, AuxRR-core, and WUN-motif, predicted in PtriZATs, function in response to MeJA, defense, low-temperatures, gibberellin, drought-inducibility, salicylic acid and auxin, which were important for plant growth under stress. Other growth regulation cis-elements, such as circadian, CAT-box, RY-element, GC-motif, AT-rich sequence, GCN4_motif, and MSA-like, were also detected, and involved in functions for circadian control, meristem expression, seed-specific regulation, anoxic specific inducibility, maximal elicitor-mediated activation, endosperm expression, and cell cycle regulation. In addition, a zinc metabolism regulation cis-element, O2-site, was detected in subgroup I PtriZATs, which implied the function of Zn2+ in PtriZATs.

3.6. Expression Patterns of PtriZAT Genes in Different Tissues and Stress Treatment

To investigate the function of PtriZAT genes the transcript abundance of PtriZATs were analyzed based on the transcription data of four growth stages, nine stress treatments, and plants of two sexes from Phytozome 13 (Figure S3). All PtriZATs were lowly expressed in all the growth stages and induced by stress treatment. The expression pattern of ten expressed PtriZATs was validated with qRT-PCR. The primer sequences for qRT-PCR are listed in Table S1. Based on the qRT-PCR analysis (Figure 4), the selected PtriZATs were highly induced by stress, especially ABA and salt. Notably, the significantly upregulated PtriZATs under abiotic stress, suggested their positive regulation, which may relate to the stress- response cis-elements (Figure 2 and Figure 4). Except for stress treatment, the expression of most PtriZATs maintained a low level during different tissues. In addition, the expression of some PtriZATs varied in different tissues, which may be because of the growth-regulation cis-elements (Figure 2 and Figure 4). At the same time, the expression pattern of some subgroup I PtriZATs (Potri.010G209400 and Potri.002G119300) were significantly induced by growth tissues such as root and stem compared to stress, which may relate to the functional complementarity caused by gene duplication events (Figure 3 and Figure 4). Interestingly, a subgroup II PtriZAT (Potri.002G119300) highly induced both growth tissues and stress, which was different from the variation of the expression of other PtriZATs. The signal and process of PtriZATs involved need more research.

3.7. Protein–Protein Interaction Networks

C2H2 ZFs may form homodimers with other transcription factors and proteins in Drosophila with long-distance interaction between the activator and reporter gene promoter, which influences protein structure and functions [31]. Protein–protein interaction network analysis was completed to investigate the regulation mechanisms of PtriZATs. The predicted protein–protein interaction of PtriZATs based on P. trichocarpa is shown in Figure 5. Some PtriZATs interacted with other PtriZATs (Table S2). Except for that case, all PtriZATs interacted with node 1 (Potri.008G195900), node 2 (Potri.005G246700), node 3 (Potri.011G168800), node 5 (Potri.001G315200), node 7 (Potri.010G019150), node 8(Potri.013G006000), node 10 (Potri.017G055200), and node 11 (Potri.018G084900). CHR910 (Potri.008G195900) was a nucleoplasmin ATPase, which is functional on the DNA helicase and histone interaction in plants [32]. HMG 20 (Potri.005G246700, Potri.011G168800) was reported to have a potential role for β-dystrobrevin in neuronal differentiation, and histone deacetylase activity regulation [33,34]. PKGII (Potri.018G084900) inhibited the proliferation of various cancer cell lines in humans [35,36,37]. MORPHEUS (Potri.013G006000) MORPHEUS (Potri.013G006000) was a plant-specific epigenetic regulator of transcriptional gene silencing and affected cytosine methylation status [38]. SWI/SNF-Related proteins (Potri.005G246700, Potri.011G168800, Potri.010G019150) regulated the progression of meiosis in male reproductive cells [39]. UFD1 (ubiquitin fusion degradation protein 1, Potri.004G163200) involved in the ubiquitin-proteasome system may interact with PtriZATs [40]. Based on the functional annotation of homologous proteins, it is possible to predict the chromatin regulation, transcriptional gene silencing, and ubiquitination- regulation function of PtriZATs.
To investigate the function of the interaction proteins of PtriZATs, we analyzed their cis-elements and expression patterns under different growth stages and stress. The specific interaction protein of Potri.010G209400, Potri.009G124900, was functional for growth regulation and all stress responses of P. trichocarpa. Potri.010G209400, a PtriZAT of subgroup I, functioned in a significant response of ABA, ACC, BAP, GA, NAA, SA, and meJA and may be related to Potri.009G124900 (Figure 6, Table S8). Most interaction proteins had no explicit comments. The cis-elements with the 2000 bp upstream of these cis-elements included many stress-response binding motifs, such as MBS (MYB binding site involved in drought-inducibility), TATC-box (gibberellin responsiveness), LTR (low-temperature responsiveness), TCA-element (salicylic acid responsiveness), ABRE (abscisic acid responsiveness), ARE (anaerobic induction), AuxRR-core (auxin responsiveness), TGACG-motif (MeJA responsiveness), P-box (gibberellin responsiveness) and WUN-motif (wound responsiveness) (Figure 7, Table S9).

3.8. The Distribution of PtriZATs in Populus Species

To investigate the distribution of ZATs in different Populus species, ZATs with two conserved ZnF-C2H2 domains in different Populus species were obtained by BLASTP using PtriZATs. The results show that different ZATs were distributed in different Populus species, and 16 ZATs were in P. deltoids, 19 ZATs were in P. euphratica, 29 ZATs were in P. alba, and 38 ZATs were in P. tomentosa (Table S10). The sequence alignment of ZATs in different Populus species had variable subunits in conserved QAGGH ZnF-C2H2 domains (Figures S4–S7, [18]). Total sequence variation of QAGGH was obtained in Podel.01G169100.1.p, Podel.10G160600.1.p, and Podel.17G095700.1.p of P. deltoids; XP_011001488.1, XP_011012172.1, and XP_011031881.1 in P. euphratica; XP_034907133.1, XP_034922750.1, and XP_034932650.1 in P. alba, KAG6741799.1, KAG6742946.1, KAG6757992.1, KAG6759880.1, KAG6780647.1, KAG6782363.1, KAG6788764.1, KAG6789197.1, KAG6792151.1 and KAG6792606.1 in P. tomentosa. Some ZATs substituted Ala for Gly of QAGGH, such as KAG6755684.1 and KAG6756859.1 in P. tomentosa. All the variable ZATs in Populus had development branches with subgroup I and subgroup II PtriZATs (Figure S8). The other Populus ZATs were divided into two subgroups with PtriZATs (Figure S8).

4. Discussion

4.1. Characteristics of PtriZATs in P. trichocarpa

We identified eleven PtriZATs with two conserved ZnF_C2H2 domains in P. trichocarpa (Figure 1, Table S3). Based on the phylogenetic tree of eleven PtriZATs, we classified them into two subgroups (Figure 2). A comparison of the protein sequences and structures revealed the variation of PtriZATs. The length of the PtriZATs varied according to subgroups. The length of ZnF-C2H2 domains of subgroup I PtriZATs (25–27 amino acids) was longer than subgroup II (24–25 amino acids) (Table 1). The location of ZnF-C2H2 domains in PtriZATs also varied according to the subgroups. The two ZnF-C2H2 domains were closer to the C-terminal in the first subtypes PtriZATs of subgroup I than subgroup II (Table 1, Figure 2). The length of spacing between the two ZnF-C2H2 domains varied from 19 to 54 amino acids, and the amino acid subunits also varied in different PtriZATs. The spacing between the core motifs of ZnF-C2H2 might be important for target sequence recognition [41], and there may be some difference in DNA-binding between different PtriZATs. The length of PtriZATs of subgroup I was also longer than subgroup II. Individual fingers of C2H2-ZF domains are specifically bound over a wide range of three base pair targets [42]. The higher quantity of ZnF-C2H2 domains and the ZnF-C2H2 DNA-binding landscapes confirmed the important role of C2H2 in the DNA binding of longer DNA sequences [43]. The length of ZnF-C2H2 domains of PtriZATs ensured the stability of a Zn finger and DNA binding ability, as reported previously [44]. The variety of spacers between the two fingers provided the necessary gaps between the core sites of the target DNA [18]. The highly conserved QALGGH motifs of PtriZATs were the same as Family C1 C2H2 of Arabidopsis and other plants, which were conserved zinc finger helices for DNA binding [18,41].

4.2. Different Distributions of ZATs in Populus Species

Different numbers of ZATs were obtained in different Populus (Table S10). The different distributions of ZATs in different Populus and plants might reflect their variation in function and evolution in Populus and plants (Tables S4 and S10). To investigate the evolutionary history of ZATs in different Populus and plants, a phylogenetic tree was built using protein sequences (Figures S2 and S8). Seven P. deltoids ZATs, seven P. euphratica ZATs, five P. alba ZATs and fourteen P. tomentosa ZATs were separated into subgroup I with subgroup I PtriZATs. Nine P. deltoids ZATs, seven P. euphratica ZATs, six P. alba ZATs, seven P. tomentosa ZATs were separated into subgroup II with subgroup II PtriZATs. The separation of most Populus ZATs showed the conservation of ZATs in Populus. To investigate the difference in independent ZATs in Populus, sequence analysis was conducted using Populus ZATs. All the independent ZATs contained variation motifs in the Zn-C2H2 domain (Figures S4–S7). C2H2 ZTFs, one of the largest gene families, were conserved in flora and fauna, the evolution of base-contacting residues for DNA binding, and the interaction of non-base-contacting residues with a DNA backbone, which plays a key role during their expansion in metazoans [45]. Sequence variation of QAGGH motifs obtained for different Populus species reflected the evolutionary events of Populus, especially the residue substitute of Gly (Figures S4–S7). The hydrophobic amino acids surrounding the motifs of ZnF-C2H2 were involved in protein–protein interaction and might interact with other DNA-binding proteins [41,46]. The total sequence variation of QAGGH in Populus species might imply larger evolutionary events and different DNA-binding functions in Populus C2H2-ZnFs (Figures S4–S7).

4.3. Chromosomal Distribution and Gene Duplication of PtriZATs

According to the chromosome location results, Potri.004G216900, Potri.006G121600, and Potri.010G229400 were possibly derived from Potri.008G032300 (Figure 3). All four PtriZATs belonged to the first subtype of Subgroup I with conserved ZnF-C2H2 domains and amino acid subunits (Figure 1 and Figure 2). The detected higher-expressed Potri.004G216900 under ABA treatment in the first subtype of subgroup PtriZATs may relate to the evolution and origin of these PtriZATs (Figure 4, Figure S3). Previous studies have identified that the Populus genome underwent at least three rounds of genome-wide duplication, followed by multiple segmental duplications, tandem duplications, and transposition events, such as retrotransposition and replicative transposition [30,47]. The origin of the four PtriZATs in the first subtype of subgroup ZATs may coincide with the genome-wide duplication. The location relationship of four Subgroup II PtriZATs was also a reflection of the genome-wide duplication, which was equalization pipeline-connected. However, the origins of other PtriZATs were unclear.

4.4. Functional Differentiation of PtriZATs

Most ZFPs take part in plant growth regulation and stress response. The ZFPs in G. hirsutum are involved in fiber cell growth and hormone response [48]. The faster and earlier response of PtaZFP2 monitored during stem bending and stress response implied its function in the growth and environmental adaption of Populus [49]. PeSTZ1, a C2H2-type zinc finger of P. euphratica, can regulate PeAPX2 to modulate ROS scavenging and enhance the freezing tolerance of Populus [13]. The higher expression of PtriZATs of subgroup II and the second subtype of subgroup I in all the stress treatments reflected the importance and wide-spectrum function of PtriZATs under stress (Figure 4 and Figure S3, Table S5). The motifs and cis-elements related to phytohormone and abiotic stress resistance identified in PtriZATs indicated their stress resistance and growth regulation functions (Tables S6 and S7; [47]). Combining the expression level and cis-element analysis showed that PtriZATs take part in the ABA, meJA, and light responses of plants. The higher expression level of PtriZATs in male plants may imply a different function of PtriZATs during sex differentiation. In P. yunnanensis Dode, there were many sex-specific responses in growth regulation and physiological metabolism [50]. Under a stress condition, Populus also shows a sex-specific response in physiological, morphological, proteome, and gene expression levels to heavy metals, salinity, drought, and nutrient deficiency [51]. During growth and stress resistance, males of Populus were more adaptive [52]. The higher expression of PtriZATs in male Populus was consistent with the strength of male plants. The interaction proteins of PtriZATs support growth regulation and the stress response function, which may relate to epigenetic mechanisms, such as histone modification [33,34], cytosine methylation [38], and ubiquitination [40]. The highly induced Potri.006G192700 and Potri.016G045500 in male plants provided the specific function of PtriZATs during sex differentiation (Figure 6, Table S8), which may be because of its function in the progression of meiosis in the male reproductive cell of SWI/SNF-Related proteins [39]. Cis-element interaction proteins contained and had a higher induced expression of PtriZATs genes, implying a function in the stress response of PtriZATs, which may occur through interaction with stress-related genes (Figure 4 and Figure 7, Table S9). Except for the functional interaction proteins of PtriZATs reported in plants, the function of other interaction proteins with a role in animals and diseases needs more research in plants [53,54] (Table S2).
Overall, the study results indicate that the PtriZATs functions were the same as the functions for DNA recognition, transcription regulation, protein folding and assembly of ZnFs in eukaryotes [2], but the mechanisms in plants need further research.

5. Conclusions

This study provided a thorough overview of the C1-2i subclass of C2H2-type Zinc Finger of P. trichocarpa and Populus. It presented a new perspective on the evolution and function of PtriZATs. The phylogenetic analysis found that eleven PtriZATs were classified into two subgroups according to their sequence characteristics of the ZnF-C2H2 domain. The phylogenetic relationship, exon-intron structure, chromosomal location, conserved motifs, and cis-regulatory elements of PtriZATs were explored in this research. The phylogenetic relationship and exon intron structure analysis supported the two subgroups classification. Chromosomal mapping and collinearity analysis revealed the duplication events of PtriZATs. Furthermore, the cis-elements analysis and transcription data of PtriZATs revealed their special expression profiles focused on stress response and sex differentiation. The validation by qRT-PCR further illustrated the function of most PtriZATs under stress, especially ABA and salt. The variation in the expression pattern of different PtriZATs may relate to functional complementation and gene duplication. The interaction proteins of PtriZATs predicted using STRING were functional as regulators of epigenetic mechanisms, which may provide clues for the functional study of PtriZATs. Our study contributes to the understanding of the structure and role of growth tissues, PtriZATs under stress, and provides resources for further functional analysis in Populus. It may contribute to improving the stress resistance of Populus using molecular biology techniques such as overexpression/mutation and regulation of epigenetic modification in future research.

Supplementary Materials

The following supporting information can be downloaded at: https://www.mdpi.com/article/10.3390/genes13101843/s1, Figure S1: Phylogenetic analysis of ZAT proteins of A. thalina and P. trichorcarpa; Figure S2: Phylogenetic analysis of ZAT proteins from different plants; Figure S3: Expression of PtriZAT genes during different growth stage and stress response; Figure S4: Multiple sequence alignment of ZAT proteins in P. alba; Figure S5: Multiple sequence alignment of ZAT proteins in P. euphratica; Figure S6: Multiple sequence alignment of ZAT proteins in P. tomentosa; Figure S7: Multiple sequence alignment of ZAT proteins in P. deltoids; Figure S8: Phylogenetic analysis of ZAT proteins of different P. species; Table S1: The primer sequences used in the study; Table S2: The predicted network of protein–protein interactions of PtriZATs; Table S3: List of PrtriZATs in P. trichocarpa; Table S4: List of ZATs in different plants; Table S5: The conserved motifs identified in PtriZATs; Table S6: The cis-regulatory elements identified in the promoters of PtriZATs; Table S7: Expression data of ZATs of P. trichocarpa; Table S8: Expression data of interaction proteins of PtriZATs in P. trichocarpa; Table S9: The cis-regulatory elements identified in the promoters of interaction proteins of PtriZATs; Table S10: List of ZATs during different Populus species.

Author Contributions

Conceptualization, investigation and Writing—original draft, P.L.; Methodology, A.Y.; Supervision, R.S.; Writing—review and editing, A.L.; All authors have read and agreed to the published version of the manuscript.

Funding

This study was supported by Yunnan Fundamental Research Projects (202201AU070072, 202201AU070205), Foundation of Yunnan Agricultural Basic Research (202101BD070001-033, 202101BD070001-126), the Project of Yunnan Provincial Department of Education Science Research Fund (2022J0503, 2021J0167, 2018JS340) and the Opening Project of Key Laboratory for Forest Resources Conservation and Utilization in the Southwest Mountains of China, Ministry of Education (KLESWFU-202010, KLESWFU-202009, KLESWFU201903).

Institutional Review Board Statement

Not applicable.

Informed Consent Statement

Not applicable.

Data Availability Statement

Not applicable.

Conflicts of Interest

The authors declare no conflict of interest.

References

  1. Miller, J.; McLachlan, A.D.; Klug, A. Repetitive zinc-binding domains in the protein transcription factor IIIA from Xenopus oocytes. EMBO J. 1985, 4, 1609–1614. [Google Scholar] [CrossRef] [PubMed]
  2. Laity, J.H.; Lee, B.M.; Wright, P.E. Zinc finger proteins: New insights into structural and functional diversity. Curr. Opin. Struct. Biol. 2001, 11, 39–46. [Google Scholar] [CrossRef]
  3. Gamsjaeger, R.; Liew, C.K.; Loughlin, F.E.; Crossley, M.; Mackay, J.P. Sticky fingers: Zinc-fingers as protein-recognition motifs. Trends Biochem. Sci. 2007, 32, 63–70. [Google Scholar] [CrossRef] [PubMed]
  4. Han, G.; Lu, C.; Guo, J.; Qiao, Z.; Sui, N.; Qiu, N.; Wang, B. C2H2 Zinc Finger Proteins: Master Regulators of Abiotic Stress Responses in Plants. Front. Plant Sci. 2020, 11, 115. [Google Scholar] [CrossRef] [Green Version]
  5. Ghosh, S.; Kant, R.; Pradhan, A.; Jha, G. RS_CRZ1, a C2H2-Type Transcription Factor Is Required for Pathogenesis of Rhizoctonia solani AG1-IA in Tomato. Mol. Plant Microbe Interact. 2021, 34, 26–38. [Google Scholar] [CrossRef]
  6. Ballerini, E.S.; Min, Y.; Edwards, M.B.; Kramer, E.M.; Hodges, S.A. POPOVICH, encoding a C2H2 zinc-finger transcription factor, plays a central role in the development of a key innovation, floral nectar spurs, in Aquilegia. Proc. Natl. Acad. Sci. USA 2020, 117, 22552–22560. [Google Scholar] [CrossRef]
  7. Arrey-Salas, O.; Caris-Maldonado, J.C.; Hernández-Rojas, B.; Gonzalez, E. Comprehensive Genome-Wide Exploration of C2H2 Zinc Finger Family in Grapevine (Vitis vinifera L.): Insights into the Roles in the Pollen Development Regulation. Genes 2021, 12, 302. [Google Scholar] [CrossRef]
  8. Chang, J.; Yu, T.; Yang, Q.; Li, C.; Xiong, C.; Gao, S.; Xie, Q.; Zheng, F.; Li, H.; Tian, Z.; et al. Hair, encoding a single C2H2 zinc-finger protein, regulates multicellular trichome formation in tomato. Plant J. 2018, 96, 90–102. [Google Scholar] [CrossRef] [Green Version]
  9. Shang, L.; Song, J.; Yu, H.; Wang, X.; Yu, C.; Wang, Y.; Li, F.; Lu, Y.; Wang, T.; Ouyang, B.; et al. A mutation in a C2H2-type zinc finger transcription factor contributed to the transition toward self-pollination in cultivated tomato. Plant Cell 2021, 33, 3293–3308. [Google Scholar] [CrossRef]
  10. Zhuang, H.; Wang, H.L.; Zhang, T.; Zeng, X.Q.; Chen, H.; Wang, Z.W.; Zhang, J.; Zheng, H.; Tang, J.; Ling, Y.H.; et al. NONSTOP GLUMES1 Encodes a C2H2 Zinc Finger Protein That Regulates Spikelet Development in Rice. Plant Cell 2020, 32, 392–413. [Google Scholar] [CrossRef]
  11. Ding, W.; Wang, Y.; Fang, W.; Gao, S.; Li, X.; Xiao, K. TaZAT8, a C2H2-ZFP type transcription factor gene in wheat, plays critical roles in mediating tolerance to Pi deprivation through regulating P acquisition, ROS homeostasis and root system establishment. Physiol. Plant 2016, 158, 297–311. [Google Scholar] [CrossRef]
  12. Cheuk, A.; Ouellet, F.; Houde, M. The barley stripe mosaic virus expression system reveals the wheat C2H2 zinc finger protein TaZFP1B as a key regulator of drought tolerance. BMC Plant Biol. 2020, 20, 144. [Google Scholar] [CrossRef] [Green Version]
  13. He, F.; Li, H.G.; Wang, J.J.; Su, Y.; Wang, H.L.; Feng, C.H.; Yang, Y.; Niu, M.X.; Liu, C.; Yin, W.; et al. PeSTZ1, a C2H2-type zinc finger transcription factor from Populus euphratica, enhances freezing tolerance through modulation of ROS scavenging by directly regulating PeAPX2. Plant Biotechnol. J. 2019, 17, 2169–2183. [Google Scholar] [CrossRef] [Green Version]
  14. Kundu, A.; Das, S.; Basu, S.; Kobayashi, Y.; Kobayashi, Y.; Koyama, H.; Ganesan, M. GhSTOP1, a C2H2 type zinc finger transcription factor is essential for aluminum and proton stress tolerance and lateral root initiation in cotton. Plant Biol. 2019, 21, 35–44. [Google Scholar] [CrossRef] [Green Version]
  15. Yu, Z.; Yan, H.; Liang, L.; Zhang, Y.; Yang, H.; Li, W.; Choi, J.; Huang, J.; Deng, S. A C2H2-Type Zinc-Finger Protein from Millettia pinnata, MpZFP1, Enhances Salt Tolerance in Transgenic Arabidopsis. Int. J. Mol. Sci. 2021, 22, 10832. [Google Scholar] [CrossRef]
  16. Zhang, S.; Liu, J.; Zhong, G.; Wang, B. Genome-Wide Identification and Expression Patterns of the C2H2-Zinc Finger Gene Family Related to Stress Responses and Catechins Accumulation in C. sinensis [L.] O. Kuntze. Int. J. Mol. Sci. 2021, 22, 4197. [Google Scholar] [CrossRef]
  17. Xie, M.; Sun, J.; Gong, D.; Kong, Y. The Roles of Arabidopsis C1-2i Subclass of C2H2-type Zinc-Finger Transcription Factors. Genes 2019, 10, 653. [Google Scholar] [CrossRef] [Green Version]
  18. Englbrecht, C.C.; Schoof, H.; Böhm, S. Conservation, diversification and expansion of C2H2 zinc finger proteins in the A. thaliana genome. BMC Genom. 2004, 5, 39. [Google Scholar]
  19. Sakamoto, H.; Araki, T.; Meshi, T.; Iwabuchi, M. Expression of a subset of the Arabidopsis Cys(2)/His(2)-type zinc-finger protein gene family under water stress. Gene 2000, 248, 23–32. [Google Scholar] [CrossRef]
  20. Van der Zaal, B.J.; Neuteboom, L.W.; Pinas, J.E.; Chardonnens, A.N.; Schat, H.; Verkleij, J.A.; Hooykaas, P.J. Overexpression of a novel Arabidopsis gene related to putative zinc-transporter genes from animals can lead to enhanced zinc resistance and accumulation. Plant Physiol. 1999, 119, 1047–1055. [Google Scholar] [CrossRef] [Green Version]
  21. Sun, Z.; Liu, R.; Guo, B.; Huang, K.; Wang, L.; Han, Y.; Li, H.; Hou, S. Ectopic expression of GmZAT4, a putative C2H2-type zinc finger protein, enhances PEG and NaCl stress tolerances in A. thaliana. 3 Biotech 2019, 9, 166. [Google Scholar] [CrossRef]
  22. Yang, K.; Li, C.Y.; An, J.P.; Wang, D.R.; Wang, X.; Wang, C.K.; You, C.X. The C2H2-type zinc finger transcription factor MdZAT10 negatively regulates drought tolerance in apple. Plant Physiol. Biochem. 2021, 167, 390–399. [Google Scholar] [CrossRef]
  23. Xing, L.; Qi, S.; Zhou, H.; Zhang, W.; Zhang, C.; Ma, W.; Zhang, Q.; Shah, K.; Han, M.; Zhao, J. Epigenomic Regulatory Mechanism in Vegetative Phase Transition of M. hupehensis. J. Agric. Food Chem. 2020, 68, 4812–4829. [Google Scholar] [CrossRef]
  24. Hall, B.G. Building phylogenetic trees from molecular data with MEGA. Mol. Biol. Evol. 2013, 30, 1229–1235. [Google Scholar] [CrossRef] [Green Version]
  25. Tamura, K.; Stecher, G.; Kumar, S. MEGA11: Molecular Evolutionary Genetics Analysis Version 11. Mol. Biol. Evol. 2021, 38, 3022–3027. [Google Scholar] [CrossRef]
  26. Chen, C.; Chen, H.; Zhang, Y.; Thomas, H.R.; Frank, M.H.; He, Y.; Xia, R. TBtools: An Integrative Toolkit Developed for Interactive Analyses of Big Biological Data. Mol. Plant 2020, 13, 1194–1202. [Google Scholar] [CrossRef]
  27. Regier, N.; Frey, B. Experimental comparison of relative RT-qPCR quantification approaches for gene expression studies in poplar. BMC Mol. Biol. 2010, 11, 57. [Google Scholar] [CrossRef] [Green Version]
  28. Deng, W.; Wang, Y.; Liu, Z.; Cheng, H.; Xue, Y. HemI: A toolkit for illustrating heatmaps. PLoS ONE 2014, 9, 111988. [Google Scholar] [CrossRef]
  29. Tippmann, H.F. Analysis for free: Comparing programs for sequence analysis. Brief Bioinform. 2004, 5, 82–87. [Google Scholar] [CrossRef]
  30. Tuskan, G.A.; Difazio, S.; Jansson, S.; Bohlmann, J.; Grigoriev, I.; Hellsten, U.; Putnam, N.; Ralph, S.; Rombauts, S.; Salamov, A.; et al. The genome of black cottonwood, P. trichocarpa (Torr. & Gray). Science 2006, 313, 1596–1604. [Google Scholar]
  31. Zolotarev, N.; Fedotova, A.; Kyrchanova, O.; Bonchuk, A.; Penin, A.A.; Lando, A.S.; Eliseeva, I.A.; Kulakovskiy, I.V.; Maksimenko, O.; Georgiev, P. Architectural proteins Pita, Zw5, and ZIPIC contain homodimerization domain and support specific long-range interactions in Drosophila. Nucleic Acids Res. 2016, 44, 7228–7241. [Google Scholar] [PubMed] [Green Version]
  32. Singh, A.K.; Saharan, K.; Baral, S.; Vasudevan, D. The plant nucleoplasmin AtFKBP43 needs its extended arms for histone interaction. Biochim. Biophys. Acta Gene Regul. Mech. 2022, 1865, 194872. [Google Scholar] [CrossRef] [PubMed]
  33. Artegiani, B.; Labbaye, C.; Sferra, A.; Quaranta, M.T.; Torreri, P.; Macchia, G.; Ceccarini, M.; Petrucci, T.C.; Macioce, P. The interaction with HMG20a/b proteins suggests a potential role for β-dystrobrevin in neuronal differentiation. J. Biol. Chem. 2010, 285, 24740–24750. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  34. Mezquita, J.; Chiva, M.; Vidal, S.; Mezquita, C. Effect of high mobility group nonhistone proteins HMG-20 (ubiquitin) and HMG-17 on histone deacetylase activity assayed in vitro. Nucleic Acids Res. 1982, 10, 1781–1797. [Google Scholar] [CrossRef]
  35. Wang, Y.; Appiah-Kubi, K.; Lan, T.; Wu, M.; Pang, J.; Qian, H.; Tao, Y.; Jiang, L.; Wu, Y.; Chen, Y. PKG II inhibits PDGF-BB triggered biological activities by phosphorylating PDGFRβ in gastric cancer cells. Cell Biol. Int. 2018, 42, 1358–1369. [Google Scholar] [CrossRef]
  36. Qian, H.; Tao, Y.; Jiang, L.; Wang, Y.; Lan, T.; Wu, M.; Pang, J.; Appiah-Kubi, K.; Chen, Y.; Wu, Y. PKG II effectively reversed EGF-induced protein expression alterations in human gastric cancer cell lines. Cell Biol. Int. 2018, 42, 435–442. [Google Scholar] [CrossRef]
  37. Wu, Y.; Cai, Q.; Li, W.; Cai, Z.; Liu, Y.; Li, H.; Pang, J.; Chen, Y. Active PKG II inhibited the growth and migration of ovarian cancer cells through blocking Raf/MEK and PI3K/Akt signaling pathways. Biosci. Rep. 2019, 39, BSR20190405. [Google Scholar] [CrossRef] [Green Version]
  38. Habu, Y. Epigenetic silencing of endogenous repetitive sequences by MORPHEUS’ MOLECULE1 in A. thaliana. Epigenetics 2010, 5, 562–565. [Google Scholar] [CrossRef] [Green Version]
  39. Sun, L.; Sun, G.; Shi, C.; Sun, D. Transcriptome analysis reveals new microRNAs-mediated pathway involved in anther development in male sterile wheat. BMC Genom. 2018, 19, 333. [Google Scholar] [CrossRef] [Green Version]
  40. Galvão, R.M.; Kota, U.; Soderblom, E.J.; Goshe, M.B.; Boss, W.F. Characterization of a new family of protein kinases from Arabidopsis containing phosphoinositide 3/4-kinase and ubiquitin-like domains. Biochem. J. 2008, 409, 117–127. [Google Scholar] [CrossRef] [Green Version]
  41. Kubo, K.; Sakamoto, A.; Kobayashi, A.; Rybka, Z.; Kanno, Y.; Nakagawa, H.; Takatsuji, H. Cys2/His2 zinc-finger protein family of petunia: Evolution and general mechanism of target-sequence recognition. Nucleic Acids Res. 1998, 26, 608–715. [Google Scholar] [CrossRef] [Green Version]
  42. Enuameh, M.S.; Asriyan, Y.; Richards, A.; Christensen, R.G.; Hall, V.L.; Kazemian, M.; Zhu, C.; Pham, H.; Cheng, Q.; Blatti, C.; et al. Global analysis of Drosophila Cys₂-His₂ zinc finger proteins reveals a multitude of novel recognition motifs and binding determinants. Genome Res. 2013, 23, 928–940. [Google Scholar] [CrossRef]
  43. Persikov, A.V.; Wetzel, J.L.; Rowland, E.F.; Oakes, B.L.; Xu, D.J.; Singh, M.; Noyes, M.B. A systematic survey of the Cys2His2 zinc finger DNA-binding landscape. Nucleic Acids Res. 2015, 43, 1965–1984. [Google Scholar] [CrossRef] [Green Version]
  44. Meseguer, A.; Årman, F.; Fornes, O.; Molina-Fernández, R.; Bonet, J.; Fernandez-Fuentes, N.; Oliva, B. On the prediction of DNA-binding preferences of C2H2-ZF domains using structural models: Application on human CTCF. NAR Genom. Bioinform. 2020, 2, 46. [Google Scholar] [CrossRef]
  45. Najafabadi, H.S.; Garton, M.; Weirauch, M.T.; Mnaimneh, S.; Yang, A.; Kim, P.M.; Hughes, T.R. Non-base-contacting residues enable kaleidoscopic evolution of metazoan C2H2 zinc finger DNA binding. Genome Biol. 2017, 18, 167. [Google Scholar] [CrossRef] [Green Version]
  46. Gill, G.; Pascal, E.; Tseng, Z.H.; Tjian, R. A glutamine-rich hydrophobic patch in transcription factor Sp1 contacts the dTAFII110 component of the Drosophila TFIID complex and mediates transcriptional activation. Proc. Natl. Acad. Sci. USA 1994, 91, 192–196. [Google Scholar] [CrossRef] [Green Version]
  47. Liu, Q.; Wang, Z.; Xu, X.; Zhang, H.; Li, C. Genome-Wide Analysis of C2H2 Zinc-Finger Family Transcription Factors and Their Responses to Abiotic Stresses in Poplar (P. trichocarpa). PLoS ONE 2015, 10, e0134753. [Google Scholar] [CrossRef] [Green Version]
  48. He, P.; Yang, Y.; Wang, Z.; Zhao, P.; Yuan, Y.; Zhang, L.; Ma, Y.; Pang, C.; Yu, J.; Xiao, G. Comprehensive analyses of ZFP gene family and characterization of expression profiles during plant hormone response in cotton. BMC Plant Biol. 2019, 19, 329. [Google Scholar] [CrossRef] [Green Version]
  49. Martin, L.; Leblanc-Fournier, N.; Azri, W.; Lenne, C.; Henry, C.; Coutand, C.; Julien, J.-L. Characterization and expression analysis under bending and other abiotic factors of PtaZFP2, a poplar gene encoding a Cys2/His2 zinc finger protein. Tree Physiol. 2009, 29, 125–136. [Google Scholar] [CrossRef] [Green Version]
  50. Chen, L.; Zhang, S.; Zhao, H.; Korpelainen, H.; Li, C. Sex-related adaptive responses to interaction of drought and salinity in Populus yunnanensis. Plant Cell Environ. 2010, 33, 1767–1778. [Google Scholar] [CrossRef]
  51. Melnikova, N.V.; Borkhert, E.V.; Snezhkina, A.V.; Kudryavtseva, A.V.; Dmitriev, A.A. Sex-Specific Response to Stress in Populus. Front. Plant Sci. 2017, 8, 1827. [Google Scholar] [CrossRef] [Green Version]
  52. Hao, L.; Chen, L.; Zhu, P.; Zhang, J.; Zhang, D.; Xiao, J.; Xu, Z.; Zhang, L.; Liu, Y.; Li, H.; et al. Sex-specific responses of Populus deltoides to interaction of cadmium and salinity in root systems. Ecotoxicol. Environ. Saf. 2020, 195, 110437. [Google Scholar] [CrossRef]
  53. Gorrec, F. The MORPHEUS protein crystallization screen. J. Appl. Crystallogr. 2009, 42, 1035–1042. [Google Scholar] [CrossRef]
  54. Xu, X.; Qiao, D.; Dong, C.; Mann, M.; Garofalo, R.P.; Keles, S.; Brasier, A.R. The SWI/SNF-Related, Matrix Associated, Actin-Dependent Regulator of Chromatin A4 Core Complex Represses Respiratory Syncytial Virus-Induced Syncytia Formation and Subepithelial Myofibroblast Transition. Front. Immunol. 2021, 12, 633654. [Google Scholar] [CrossRef]
Genes 13 01843 g001 550
Figure 1. Sequence alignment and structure analysis of PtriZATs. (A). Multiple sequence alignment of PtriZAT proteins with BioEdit. Blue label and letters denote domains of PtriZAT proteins. The codes for shades are: Black, >50% conservation position with BioEdit; Green, same amino acid subunits; Yellow, characteristic bases of C1-2i ZEPs of A. thalina [18]. (B,C). Protein structure of ZnF-C2H2 domains in Potri.004G216900 and Potri.001G295500 using Expasy-ProtParam. Potri.004G216900 model was built using 6ml2.1.A template with 2.7Å X-ray method (0.30 seq similarity, 0.37 coverage, 120–233 range); Potri.001G295500 model was built using 6ml2.1.A template with 1.87Å X-ray method (0.30 seq similarity, 0.36 coverage, 63–148 range).
Figure 1. Sequence alignment and structure analysis of PtriZATs. (A). Multiple sequence alignment of PtriZAT proteins with BioEdit. Blue label and letters denote domains of PtriZAT proteins. The codes for shades are: Black, >50% conservation position with BioEdit; Green, same amino acid subunits; Yellow, characteristic bases of C1-2i ZEPs of A. thalina [18]. (B,C). Protein structure of ZnF-C2H2 domains in Potri.004G216900 and Potri.001G295500 using Expasy-ProtParam. Potri.004G216900 model was built using 6ml2.1.A template with 2.7Å X-ray method (0.30 seq similarity, 0.37 coverage, 120–233 range); Potri.001G295500 model was built using 6ml2.1.A template with 1.87Å X-ray method (0.30 seq similarity, 0.36 coverage, 63–148 range).
Genes 13 01843 g001
Genes 13 01843 g002 550
Figure 2. Phylogenetic tree, motifs and structure of PtriZATs. (A). The phylogenetic tree of PtriZATs constructed on the basis of the maximum-likelihood method. (B). The conserved motifs of PtriZATs predicted using various Multiple Em for Motif Elicitation (MEME). The colored boxes represented 15 conserved motifs, the grey lines are non-conserved sequences. (C). A schematic diagram showing the ZnF-C2H2 domains of PtriZATs. The green boxes exhibited the ZnF-C2H2 domains. (D). Cis-elements of PtriZATs during the 2000bp upstream sequences. (E). Gene structures of PtriZAT genes. The yellow box showed the CDS, green ones were no-coding sequences.
Figure 2. Phylogenetic tree, motifs and structure of PtriZATs. (A). The phylogenetic tree of PtriZATs constructed on the basis of the maximum-likelihood method. (B). The conserved motifs of PtriZATs predicted using various Multiple Em for Motif Elicitation (MEME). The colored boxes represented 15 conserved motifs, the grey lines are non-conserved sequences. (C). A schematic diagram showing the ZnF-C2H2 domains of PtriZATs. The green boxes exhibited the ZnF-C2H2 domains. (D). Cis-elements of PtriZATs during the 2000bp upstream sequences. (E). Gene structures of PtriZAT genes. The yellow box showed the CDS, green ones were no-coding sequences.
Genes 13 01843 g002
Genes 13 01843 g003 550
Figure 3. The chromosomal location and gene duplication events of PtriZAT genes. (A). Chromosomal location of PtriZAT genes in P. trichocarpa. PtriZAT genes were widely mapped to 8 of the 19 Populus chromosomes. (B). The gene duplication events of PtriZATs. The paralogous pairs of PtriZAT gene in the segmental duplicated blocks were connected with gray lines. Chromosome numbers were indicated at the side of each line.
Figure 3. The chromosomal location and gene duplication events of PtriZAT genes. (A). Chromosomal location of PtriZAT genes in P. trichocarpa. PtriZAT genes were widely mapped to 8 of the 19 Populus chromosomes. (B). The gene duplication events of PtriZATs. The paralogous pairs of PtriZAT gene in the segmental duplicated blocks were connected with gray lines. Chromosome numbers were indicated at the side of each line.
Genes 13 01843 g003
Genes 13 01843 g004 550
Figure 4. Expression of PtriZAT genes under stress treatment and different tissues. EF1 was used as an internal control. Data are means of three biological replicates and error bars are ± SE from three independent experiments, each performed with 2–3 leaves from three separate plants, asterisks indicate significant differences by Tukey LSD test (* p < 0.05, ** p < 0.01).
Figure 4. Expression of PtriZAT genes under stress treatment and different tissues. EF1 was used as an internal control. Data are means of three biological replicates and error bars are ± SE from three independent experiments, each performed with 2–3 leaves from three separate plants, asterisks indicate significant differences by Tukey LSD test (* p < 0.05, ** p < 0.01).
Genes 13 01843 g004
Genes 13 01843 g005 550
Figure 5. The predicted network of protein–protein interactions of PtriZATs by STRING. The different colors represent different types of interactions. The interaction proteins were as follows: 1, Potri.008G195900; 2, Potri.005G246700; 3, Potri.011G168800; 4, Potri.001G417300; 5, Potri.001G315200; 6, Potri.004G216900; 7, Potri.010G019150; 8, Potri.013G006000; 9, Potri.013G007800; 10, Potri.017G055200; 11, Potri.018G084900; 12, Potri.008G032300; 13, Potri.004G163200; 14, Potri.009G124900; 15, Potri.010G209400; 16, Potri.006G192700; 17, Potri.016G045500; 18, Potri.001G235800;19, Potri.009G027700; 20, Potri.001G143700; 21, Potri.001G173200; 22, Potri.001G295500; 23, Potri.009G089400; 24, Potri.002G119300; 25, Potri.014G017300; 26, Potri.010G229400.
Figure 5. The predicted network of protein–protein interactions of PtriZATs by STRING. The different colors represent different types of interactions. The interaction proteins were as follows: 1, Potri.008G195900; 2, Potri.005G246700; 3, Potri.011G168800; 4, Potri.001G417300; 5, Potri.001G315200; 6, Potri.004G216900; 7, Potri.010G019150; 8, Potri.013G006000; 9, Potri.013G007800; 10, Potri.017G055200; 11, Potri.018G084900; 12, Potri.008G032300; 13, Potri.004G163200; 14, Potri.009G124900; 15, Potri.010G209400; 16, Potri.006G192700; 17, Potri.016G045500; 18, Potri.001G235800;19, Potri.009G027700; 20, Potri.001G143700; 21, Potri.001G173200; 22, Potri.001G295500; 23, Potri.009G089400; 24, Potri.002G119300; 25, Potri.014G017300; 26, Potri.010G229400.
Genes 13 01843 g005
Genes 13 01843 g006 550
Figure 6. Expression of interaction proteins of PtriZATs encoded genes during different growth stages and stress response. The expression data of 15 PtriZAT genes were from Phytozome13. The sex differentiation samples including early and late growth of female and male plants. The samples of different tissues including bud (apical, predormant, leaf dormant, swelling, early dormant, fully open), leaf (young, immature), root (tip), steam (inode, node). The nine stress treatments include ABA, ACC, BAP, BL, GA, NAA, SA, SL and meJA. The color scale represents the value of Log2(FPKM).
Figure 6. Expression of interaction proteins of PtriZATs encoded genes during different growth stages and stress response. The expression data of 15 PtriZAT genes were from Phytozome13. The sex differentiation samples including early and late growth of female and male plants. The samples of different tissues including bud (apical, predormant, leaf dormant, swelling, early dormant, fully open), leaf (young, immature), root (tip), steam (inode, node). The nine stress treatments include ABA, ACC, BAP, BL, GA, NAA, SA, SL and meJA. The color scale represents the value of Log2(FPKM).
Genes 13 01843 g006
Genes 13 01843 g007 550
Figure 7. Cis-elements of PtriZATs interaction proteins during the 2000 bp upstream sequences. The color labels were on the right, the cis-elements message seen on Table S9.
Figure 7. Cis-elements of PtriZATs interaction proteins during the 2000 bp upstream sequences. The color labels were on the right, the cis-elements message seen on Table S9.
Genes 13 01843 g007
Table
Table 1. Characteristics of PtriZAT proteins.
Table 1. Characteristics of PtriZAT proteins.
ID.Number of Amino AcidsZn-C2H2 Domain1Zn-C2H2 Domain2Molecular WeightTheoretical pIAliphatic IndexGrand Average of Hydropathicity (GRAVY)Location
Potri.001G235800.1.p19855–80101–12721,440.739.6277.02−0.399nucle-
Potri.002G119300.1.p 25293–117146–17127,162.327.759.68−0.57nucle-
Potri.004G216900.1.p310129–155209–23433,781.647.2362.03−0.695nucle-
Potri.006G121600.2.p250184–209113–13927,202.539.0163.24−0.63nucle-
Potri.008G032300.1.p303125–151202–22833,762.197.7455.38−0.938nucle-
Potri.009G027700.1.p19351–7699–12321,035.399.5776.89−0.41nucle-
Potri.009G089400.1.p25080–105132–15726,305.148.8355.12−0.657nucle-
Potri.010G209400.1.p17946–7291–11620,059.969.0661.62−0.523nucle-
Potri.010G229400.1.p302121–147199–22333,286.637.2155.93−0.901nucle-
Potri.014G017300.1.p24891–115146–17126,605.778.458.27−0.56nucle-
Potri.001G295500.1.p24067–92122–14725,363.268.4556.62−0.577nucle-
Publisher’s Note: MDPI stays neutral with regard to jurisdictional claims in published maps and institutional affiliations.

Share and Cite

MDPI and ACS Style

Li, P.; Yu, A.; Sun, R.; Liu, A. Function and Evolution of C1-2i Subclass of C2H2-Type Zinc Finger Transcription Factors in POPLAR. Genes 2022, 13, 1843. https://doi.org/10.3390/genes13101843

AMA Style

Li P, Yu A, Sun R, Liu A. Function and Evolution of C1-2i Subclass of C2H2-Type Zinc Finger Transcription Factors in POPLAR. Genes. 2022; 13(10):1843. https://doi.org/10.3390/genes13101843

Chicago/Turabian Style

Li, Ping, Anmin Yu, Rui Sun, and Aizhong Liu. 2022. "Function and Evolution of C1-2i Subclass of C2H2-Type Zinc Finger Transcription Factors in POPLAR" Genes 13, no. 10: 1843. https://doi.org/10.3390/genes13101843

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

Article Metrics

Back to TopTop