Skip to main content
Download PDF

Molecular characterization of PSEUDO RESPONSE REGULATOR family in Rosaceae and function of PbPRR59a and PbPRR59b in flowering regulation

BMC Genomics volume 25, Article number: 794 (2024) Cite this article

Abstract

Background

PSEUDO RESPONSE REGULATOR (PRR) genes are essential components of circadian clock, playing vital roles in multiple processes including plant growth, flowering and stress response. Nonetheless, little is known about the evolution and function of PRR family in Rosaceae species.

Results

In this study, a total of 43 PRR genes in seven Rosaceae species were identified through comprehensive analysis. The evolutionary relationships were analyzed with phylogenetic tree, duplication events and synteny. PRR genes were classified into three groups (PRR1, PRR5/9, PRR3/7). The expansion of PRR family was mainly derived from dispersed and whole-genome duplication events. Purifying selection was the major force for PRR family evolution. Synteny analysis indicated the existence of multiple orthologous PRR gene pairs between pear and other Rosaceae species. Moreover, the conserved motifs of eight PbPRR proteins supported the phylogenetic relationship. PRR genes showed diverse expression pattern in various tissues of pear (Pyrus bretschneideri). Transcript analysis under 12-h light/ dark cycle and constant light conditions revealed that PRR genes exhibited distinct rhythmic oscillations in pear. PbPRR59a and PbPRR59b highly homologous to AtPRR5 and AtPRR9 were cloned for further functional verification. PbPRR59a and PbPRR59b proteins were localized in the nucleus. The ectopic overexpression of PbPRR59a and PbPRR59b significantly delayed flowering in Arabidopsis transgenic plants by repress the expression of AtGI, AtCO and AtFT under long-day conditions.

Conclusions

These results provide information for exploring the evolution of PRR genes in plants, and contribute to the subsequent functional studies of PRR genes in pear and other Rosaceae species.

Peer Review reports

Background

The circadian clock system of plants is an endogenous timing mechanism derived from adaptation to day/ night cycles of the environment during the long evolutionary process. Through the circadian clock system, plants are able to sense and predict the dynamics of environmental changes and complete critical growth and development processes at the right time [1, 2]. In recent decades, numerous studies have found that physiological activities, such as stomatal movement, leaf motion, flower opening and closure, hypocotyl elongation, photoperiodic flowering, photosynthesis, stress resistance and immune response, exist circadian rhythms and are regulated by circadian clock [3,4,5,6,7,8]. The central oscillator of clock system is composed of transcriptional‐translational feedback loops, in which CCA1 (CIRCADIAN CLOCK ASSOCIATED 1), LHY (LATE ELONGATED HYPOCOTYL), PRRs (PSEUDO RESPONSE REGULATORs), ELF3 (EARLY FLOWERING 3), ELF4, LUX (LUX ARRHYTHMO) and other clock-related genes are play critical roles [9]. Not only in Arabidopsis (Arabidopsis thaliana), more and more clock-related genes involved in key agricultural traits have been discovered and utilized [10, 11].

In 1995, the core clock mutant, toc1, was identified in Arabidopsis [12]. In 2000, AtTOC1 (TIME OF CAB EXPRESSION 1, also called PRR1) was isolated, and the first feedback loop of a plant central oscillator was established between AtCCA1/LHY and AtTOC1 in 2001 [13]. Subsequently, four PRR genes (AtPRR3, AtPRR5, AtPRR7, and AtPRR9) were characterized to participate in the formation of other feedback loops [14,15,16]. As core components of the circadian clock, five PRR genes show robust rhythmic expressions with a near 24 h period. From dawn to evening, the transcriptional levels of AtPRR9/AtPRR7/AtPRR5/AtPRR3/AtPRR1 accumulate sequentially and peak 2 h to 3 h intervals [17]. Arabidopsis prr mutants display altered phenotypes, such as late flowering, decreased growth, and increased drought and cold stress resistance [18,19,20,21]. CO (CONSTANT) is the key element of photoperiodic flowering, and circadian clock genes control the dynamics of CO from multiple levels such as transcription and translation [22]. PRR9, PRR7, and PRR5 promote flowering by activating CO expression during the daytime [21], or by interacting with CO proteins to mediate its accumulation [23].

Members of the PRR gene family contribute greatly to the clock system and serve as vital components. PRRs regulates gene expression by forming protein complexes, and integrates information such as light and temperature in the clock system [24, 25]. Given the influence of clock systems on photoperiodic responses such as flowering, PRR genes are found to have mutants that alter flowering timing or affect photoperiodic sensitivity [11, 24, 25]. PRR homologous genes have also been identified in other plant species, including monocotyledons such as rice (Oryza sativa) [26], maize (Zea mays) [27], wheat (Triticum aestivum) [28] and cotton (Gossypium hirsutum) [29], and dicotyledons such as soybean (Glycine max) [30], rose (Rosa chinensis) [31] and Chrysanthemum morifolium [32]. These PRR proteins have two highly conserved structures with a psREC (pseudo receiver) domain at the N-terminus and a CCT (CONSTANS, CO-like, and TOC1) motif at the C-terminus. Based on phylogenetic relationships and similarities to Arabidopsis proteins, the PRR family is divided into three clades, including PRR1, PRR3/7 and PRR5/9 [25]. Circadian researches have gradually shifted to more valuable crops, and in-depth studies on PRR gene function have been carried out in a variety of crop species [10, 11]. For example, BvBTC1 (BOLTING TIME CONTROL 1), which belongs to the PRR family, interacts with BvBBX19 (B-BOX 19) to achieve CO function, inducing beet flowering by regulating downstream target gene BvFT1 (FLOWERING LOCUS T 1) and BvFT2 [33, 34]. In soybean, GmPRR3a and GmPRR3b are involved in photoperiodic flowering, and GmPRR3b have been selected for geographic expansion during domestication [35, 36]. In addition, OsPRR37 in rice [37], SbPRR37 in sorghum (Sorghum bicolor) [38], and HvPRR3 in barley (Hordeum vulgare) [39] play an important role in controlling flowering time.

Members of the PRR gene family have been identified in many plants [33,34,35,36,37,38,39]. However, few studies have explored these genes and their functions in fruit crops. Rosaceae contains several economically valuable fruit crops, representing species such as pear (Pyrus bretschneideri), apple (Malus domestica), peach (Prunus persica), strawberry (Fragaria vesca), Japanese apricot (Prunus mume), sweet cherry (Prunus avium) and black raspberry (Rubus occidentalis). Moreover, the genome of these plants has been sequenced and released. Pear is widely cultivated worldwide, and flowering is the basis for the formation of pear fruit. As noted previously, PRR genes involved in flowering regulation, but the molecular characterizations of the PRRs in pear and other Rosaceae species have not been studies in detail. In this study, we identified 43 members of PRR family from seven Rosaceae species, and systematically analyzed their phylogenetic relationship, classification, conserved domain, chromosomal location, and evolutionary history. Furthermore, the expression patterns, subcellular localization, and flowering phenotypes of PbPRRs were conducted. We found that PbPRR59a and PbPRR59b may be involved in circadian and photoperiodic responses and influence flowering time. The results of this work provide a basic for further elucidating the functions of PRRs in Rosaceae species.

Results

Genome-wide identification and classification of PRR members in seven Rosaceae species

To identify the members of PRR family in the genomes of seven Rosaceae species, five PRR (AtPRR1/ AtPRR3/ AtPRR5/ AtPRR7/ AtPRR9) protein sequences of Arabidopsis were used as query for BLASTP search. The transcripts of the same gene were removed, and the conserved domains of the sequences were identified by NCBI CD-Search tool to obtain the final PRR members. In this study, 43 PRR candidate genes from seven Rosaceae species were confirmed, including eight in pear, eight in apple, nine in peach, four in strawberry, four in Japanese apricot, five in sweet cherry, and five in black raspberry (Fig. 1 and Table S1). The 43 putative proteins, like the known PRRs, have the N-terminal psREC domain and the C-terminal CCT domain, with less conserved intermediate sequences (Fig. 1).

Fig. 1
figure 1

Phylogenetic relationships and conserved domains of the PRR proteins in the seven Rosaceae species and Arabidopsis. The pink, blue, and orange blocks represent groups I, II, and III respectively. Green and purple rectangles outside the circle represent psREC and CCT conserved domains, respectively

Full size image

To investigate the evolutionary relationships of PRR members in these representative species of Rosaceae, a phylogenetic tree was generated using all protein sequences. These PRR homologous genes were categorized into group I (PRR1)、group II (PRR5/9) and group III (PRR3/7) according to their similarity with Arabidopsis (Fig. 1). PRR members of different species were distributed in all three groups. Phylogenetic analysis showed that PRR genes of pear and apple were clustered in the same clade indicating their close relationships.

Furthermore, the genetic characteristics of each PRR were analyzed, including the position of the gene on a chromosome, protein sequence length, protein molecular weight, and isoelectric point (Table S1). The length of majority PRR proteins were between 500 and 800 amino acids. The protein molecular weight of 43 PRR proteins ranged from 53.32 to 115.57 kDa, and the isoelectric point ranged from 5.16 to 8.74. Of the 43 genes, 40 genes were randomly distributed on chromosomes. In details, six of the eight PRR genes were anchored onto five of the 17 chromosomes in pear, and two were located on the scaffolds. In Japanese apricot, chromosomes 1, 5, and 7 each harbored a PRR gene, and the remaining one was located on scaffold1366. Eight PRR genes were mapped onto six chromosomes in apple, and nine PRR genes were mapped onto three chromosomes in peach. In strawberry, two genes were located on chromosome 7, and one gene was mapped onto each of chromosome 5 and 6. Five PRR genes were distributed on Chr2, Chr5 and Chr6 in sweet cherry. Five PRR genes were distributed on Chr5, Chr6 and Chr7 in black raspberry.

Gene duplication events and synteny analysis of PRR gene family in seven Rosaceae species

Gene duplication events have contributed to gene family evolution and gene function diversification [40]. Gene duplication events of the PRR family in seven Rosaceae species were analyzed using DupGen_finder pipeline software [41]. A total of 51 duplicated gene pairs were found that were assigned to four common events, including DSD (dispersed duplication), WGD (whole-genome duplication), TD (tandem duplication), and TRD (transposed duplication), while PD (proximal duplication) were not detected (Fig. 2). DSD-derived gene pairs existed in all seven Rosaceae species, and the number accounted for 56.86% (29 gene pairs) of all pairs. Except strawberry and Japanese apricot, some gene pairs of the other five species were derived from WGD event, accounting for 35.29% (18 gene pairs) of the total (Table S2). Only DSD- and WGD-derived gene pairs were found in pear and apple, suggesting that they might contribute to the evolution of the corresponding PRR family. Peach and sweet cherry had the same modes of gene duplication events, consisting of DSD (3 gene pairs), TD (1 gene pair), and WGD (1 gene pair). DSD was identified as the only driving force for PRR family in strawberry. In addition, one pair of duplicated gene in Japanese apricot and one in black raspberry were derived from TRD event (Fig. 2 and Table S2).

Fig. 2
figure 2

Gene duplication events of the PRR family in the seven Rosaceae species. Statistical results of the number (a) and percentage (b) of gene pairs driven by different types of duplication events in each species. Duplication events include DSD (dispersed duplication, green), WGD (whole-genome duplication, blue), TD (tandem duplication, pink), and TRD (transposed duplication, orange), each represented by a different colored bar

Full size image

In molecular evolution, Ks (synonymous substitution rate) and Ka (non-synonymous substitution rate) are fundamental parameters for estimating selection tendencies between homologous genes, where Ks is generally used to understand the timing of evolutionary divergence [42, 43]. In this study, the Ks values of WGD-derived gene pairs ranged from 0.02 to 2.58 in pear, 0.17 to 2.93 in apple, and 1.43 to 1.97 in black raspberry (Table S3). The Ks value of one WGD-derived gene pair in peach was 1.31, and one in sweet cherry was 1.35. Previous study has shown that the pear genome has experienced two rounds of WGD events, occurring at 30–45 million years ago (Ks = 0.15–0.30) and ∼140 million years ago (Ks = 1.50–1.80) [44]. In detail, the Ks values of four WGD-derived gene pairs in pear were between 0.15 and 0.30, indicating that the divergent time of these PbPRR paralogs were during the recent WGD event. Ka/Ks ratio greater than one or less than one represents different selection pressure. Moreover, the ratios of all PRR duplicated gene pairs in seven Rosaceae species were less than one, suggesting that purifying selection was the main driving force for PRR family evolution in Rosaceae species (Table S3).

Paralogous PRR gene pairs in seven Rosaceae species were analyzed above, and further orthologous PRR gene pairs between pear and other six species were identified by McScanx [45]. Excluding the PRR genes located on scaffolds, 49 gene pairs had syntenic relationships (Fig. 3). The number of PRR gene pairs between pear and apple was the highest with 12 pairs, followed by 10 pairs between pear and black raspberry. In addition, there were 8, 7, 6, and 6 interspecies syntenic gene pairs between pear and strawberry, sweet cherry, peach and Japanese apricot. The results suggested that PRR genes in seven Rosaceae species had strong homology and conserved relationship.

Fig. 3
figure 3

Syntenic relationships of PRR gene pairs between pear and six Rosaceae species. The curved boxes of different colors represent the chromosomes of the seven species, and the curved lines of corresponding colors represent the PPR gene pairs between the corresponding species and pear. The short red lines outside the circles represent the approximate locations of PRR genes

Full size image

Conserved motif and gene structure analysis of PRR genes in pear

To comprehension the characteristics and functions of PRR genes in pear, conserved motif and gene structure were performed using MEME and GSDS online software. Eight PbPRR genes were named based on AtPRR genes in phylogenetic tree. The results of MEME analysis showed that PbPRR and AtPRR proteins in the same group had similar motif composition, which supported the phylogenetic relationship (Fig. 4a). Motifs 1, 3, and 4 were present in all PbPRR proteins, which represented the conserved pseudo receiver domain at the N-terminus. Motif 2 were ubiquitous in all members and identified as the CCT domain. Whereas group I only had motifs 1–4, group II and III had more diverse motifs. For example, each member of group II and III contained motif 6. Except for AtPRR9 and PbPRR3, motif 9 was detected in most group II and III proteins. In addition to the motifs shared with AtPRR7, four PbPRRs in group III possessed special motifs 7 and 8, suggesting that they may have functional divergence.

Fig. 4
figure 4

Conserved motif and gene structure analysis of PRR family in Arabidopsis and pear. a Conserved motif compositions of PbPRR and AtPRR proteins. Ten motifs identified by MEME are represented by rounded rectangles of different colors. b Exon–intron structures of PbPRR and AtPRR genes. Blue rounded rectangles, green rounded rectangles, and black lines represent UTRs (untranslated region), exons and introns, respectively. The members of PbPRR and AtPRR are marked with red and blue dots, respectively. The scales represent the length of the protein and genomic sequence, respectively

Full size image

The results of gene structure analysis showed that all PRR members contain multiple exons and introns (Fig. 4b). In group I, both PbTOC1a and PbTOC1b had six exons, the same number as AtTOC1. The exon number of PbPRR59a (8) and PbPRR59b (8) were more than AtPRR5 (6) and AtPRR9 (7) in group II, while PbPRR3 (8) was less than AtPRR3 (9) in group III. Despite smaller fluctuations in exon number, the same groups still had similar gene structures. Taken together, these evidences indicated that some members of the PbPRR family have conservative functions similar to AtPRRs, and others may have different roles.

Expression analysis of PbPRR genes

To obtain more information about the biological functions of PbPRRs, gene expression patterns were analyzed using qRT-PCR assay. First, we examined the expression levels of eight PbPRR genes in vegetative and reproductive organs, including root, stem, leaf, leaf bud, flower bud, petal, anther and ovary (Fig. 5). The relative expression levels of PbTOC1a and PbTOC1b were higher in root and ovary than in other organs. PbPRR59a and PbPRR59b had a similar expression pattern with extremely high levels in root and stem. The transcription levels of three PbPRR7 homologous genes were higher in vegetative organs, and lower in reproductive organs except petal. Unlike the other seven PbPRR genes which exhibited a predominant expression in root, more PbPRR3 transcripts were accumulated in leaf bud.

Fig. 5
figure 5

Expression analysis of PbPRR genes in different tissues. The gray columns represent vegetative organs including root, stem, leaf, and leaf bud, while the black columns represent reproductive organs including flower bud, petal, anther, and ovary. The relative expression was calculated using PbUBQ as the reference gene. The maximum expression of each gene was set to “1” for standardized calculation. Data are means of three replicates with standard error. Different letters above the columns represent significant differences (P < 0.05) using one-way ANOVA Tukey’s multiple range tests

Full size image

In Arabidopsis, PRR genes are key components of circadian clock [9], and increasing evidence shows that the expression pattern of PRR genes in other species also present rhythmic diurnal oscillation nearly 24 h [27, 29, 30]. Eight PbPRR genes were clearly detected in the pear leaves, which are the primary site for sensing diurnal changes. Next, we examined the expression changes of PbPRR genes in pear leaves under 12-h light/12-h dark condition (Fig. 6). All PbPRR genes exhibited obvious rhythmic diurnal patterns during a light/ dark cycle. Transcription levels of PbTOC1a and PbTOC1b dropped steeply after dawn (zeitgeber time 5; ZT 5), gradually rose throughout the day, and rapidly accumulated to peak before dawn (ZT 21). In contrast, transcripts of the remaining PbPRR genes peaked at 9 h (ZT 9) after exposure to light. For example, both PbPRR59a and PbPRR59b remained low expression levels in the morning and evening, with higher detected only in the afternoon (ZT 9- ZT 13).

Fig. 6
figure 6

Expression patterns of PbPRR genes under 12-h light/12-h dark conditions. The initial exposure to light is defined as zeitgeber time zero (ZT 0). Starting from ZT1, leaf samples were collected 4 h intervals in the given 24 h. White and gray backgrounds indicate light and dark treatment, respectively. The relative expression was calculated using PbUBQ as the reference gene. The maximum expression of each gene was set to “1” for standardized calculation. Data are means of three replicates with standard error

Full size image

To investigate the clock properties of PbPRR genes, we examined their expression profiles in pear leaves under constant light conditions. For three days, PbPRR genes except PbPRR3 still showed stable patterns of rhythmic expression, implying that they were clock-related genes (Fig. 7). The dynamics of the first day were similar to the 12-h light/12-h dark condition, with PbPRRs peaking at the corresponding time point. On the second and third days, they maintained the same rhythm, but the expression period was longer and the expression amplitudes were reduced due to the continuous light treatment.

Fig. 7
figure 7

Expression patterns of PbPRR genes under constant light conditions for three days. The initial exposure to light is defined as zeitgeber time zero (ZT 0). Starting from ZT1, leaf samples were collected 4 h intervals in the given 72 h. White and light gray backgrounds indicate the alternation of subjective day and night. The relative expression was calculated using PbUBQ as the reference gene. The maximum expression of each gene was set to “1” for standardized calculation. Data are means of three replicates with standard error

Full size image

Subcellular localization of PbPRR59a and PbPRR59b proteins

In Arabidopsis, PRR proteins are localized in the nucleus and act as transcription factors to regulate gene expression [17, 46]. To further study potential functions of PbPRR59a and PbPRR59b, we detected their subcellular localization in epidermal cells of tobacco leaves. The full-length coding regions of PbPRR59a and PbPRR59b were used to construct fusion proteins with GFP (green fluorescent protein), respectively. Transient expression assay showed that the fluorescent signals of PbPRR59a-GFP and PbPRR59b-GFP fusion proteins were observed only in the nucleus (Fig. 8).

Fig. 8
figure 8

Subcellular localization of PbPRR59a and PbPRR59b proteins in tobacco epidermal cells. Green represents GFP signal from the GFP-fusion proteins. Blue represents DAPI fluorescence as the nuclear localization marker. Merge represents superimposed GFP, DAPI and bright field images. Vector represents the control using 35S: GFP empty vector. Bar = 10 μm

Full size image

Ectopic overexpression of PbPRR59a and PbPRR59b delayed flowering in Arabidopsis under long-day conditions

Because the stable genetic transformation system of pear has not been established to observe the flowering phenotype, heterologous transgenic materials of Arabidopsis were used to explore the influence of genes on flowering. The full-length coding sequences of PbPRR59a and PbPRR59b were placed into constitutive CaMV 35S promoter-driven vectors, and these constructs were introduced into wild-type Arabidopsis (Col-0), respectively. The PbPRR59a and PbPRR59b independent transgenic lines were identified through semi-quantitative RT-PCR analysis and participated in subsequent phenotypic observation (Fig. 9b).

Fig. 9
figure 9

Overexpression of PbPRR59a and PbPRR59b delayed flowering in Arabidopsis under LD conditions. a Flowering time phenotypes of vector control plants, PbPRR59a- and PbPRR59b-overexpression transgenic lines under long-day conditions (16-h light/8-h dark). b Identification of PbPRR59a and PbPRR59b transgenic lines using semi-quantitative RT-PCR and gene-specific primers shown in table S4. c Days to first flowering and number of corresponding rosette leaf of transgenic lines and control plants. Data are means with standard error (n ≥ 13). Different letters above the columns represent significant differences (P < 0.05) using one-way ANOVA Tukey’s multiple range tests. d Transcript levels of AtGI, AtCO, and AtFT in PbPRR59a and PbPRR59b transgenic lines. Data are means of three replicates with standard error. The relative expression levels were normalized to AtACTIN, and the maximum expression of each gene was set to “1”. ** indicates P < 0.01 and *** indicates P < 0.001 using Student’s t-tests compared with vector control plants

Full size image

Cultured from seed under long-day (16-h light/8-h dark) conditions, PbPRR59a and PbPRR59b overexpression (OE) transgenic plants exhibited a delayed flowering phenotype compared to the empty vector control plants (Fig. 9a). We measured the physiological indexes of these plants, including the time of the first flower opening after bolting and the corresponding number of rosette leaf. In detail, both PbPRR59a-OE and PbPRR59b-OE lines took more than 35.70 days to open their first flower on average, compared to 32.79 days for control plants (Fig. 9c). Simultaneously, the mean number of rosette leaf also increased significantly in transgenic lines. To further investigate the underlying cause of PbPRR59a and PbPRR59b on flowering, the expression levels of endogenous flowering time-related genes in different lines were examined by qRT-PCR assay. The transcripts of these key genes, including AtGI, AtCO and AtFT, were significantly reduced in both PbPRR59a and PbPRR59b transgenic lines than in control plants (Fig. 9d). The results implied that PbPRR59a and PbPRR59b might negatively regulate flowering time by inhibiting the expression of flowering related genes.

Discussion

The PRR family is a small gene family that belongs to a clade of CCT family and is conserved in plants [47]. PRR genes are involved in maintaining the stable operation of circadian clock and play important roles in transition from vegetative growth to reproductive growth in plants [24, 25]. However, detailed research on the PRR family of Rosaceae plants is still scarce. In this study, we identified 43 PRR genes from seven Rosaceae species and analyzed their evolutionary relationships through phylogenetic tree, duplication event, and syntenic relationship. Moreover, the gene structure, conserved domain and expression profile of eight PRR genes in pear were investigated. Transgenic plants were used to verify that PbPRR59a and PbPRR59b may be involved in flowering regulation as repressors.

Genome-wide identification and characterization of PRR family in more than twenty species has proved that PRR genes are well conserved in plant evolution [24, 27,28,29,30, 48, 49]. At least one PRR member is present in the original single-celled green plant (e.g. Chlamydomonas reinhardtii), in the liverwort (e.g. Marchantia polymorpha) and moss (e.g. Physcomitrella patens), in the fern (e.g. Selaginella moellendorffii), and in the gymnosperm (e.g. Picea abies) and angiosperms [24, 49]. The numbers of PRR genes are often greater in angiosperms than in other plants [25]. In this study, the PRR families of seven Rosaceae species were investigated, with the number of genes distributed between 4 and 9, which is close to that of many reported angiosperms, such as Arabidopsis (5), rose (5) [31], and poplar (7) (Populus trichocarpa) [50]. The PRR1 (TOC1) clade of the PRR family contains only one gene in most plants, such as dicotyledonous representative Arabidopsis [17] and monocotyledonous representative rice [26]. However, two PRR1 homologous genes were found in four of the seven Rosaceae species, all of which were gene pairs. Gene and genome duplication are major forces driving gene family expansion and biodiversity. The contribution of five duplication events (WGD, TD, PD, TRD and DSD) varies across species [41]. PbTOC1a and PbTOC1b in pear were WGD-derived gene pair, which were also present in apple, while the two homologs of PRR1 in peach and sweet cherry were both TD-derived. In addition to Rosaceae species, additional gene copies of PRR1 have also been found in soybeans and maize [27, 30], and the potential functions of these homologous genes that have been retained in the long evolutionary process need to be further elucidated.

As previously reported in other species [25], the 43 PRR genes identified in Rosaceae were well divided into three groups, all of which had N-terminal and C-terminal conserved domains. The characteristics of PbPRR and AtPRR protein sequences showed that the motif composition in the same group were similar, while were distinctly among groups. The divergence of the PRR group holds potential important implications for understanding evolution of clock and its adaptation to environmental cues. Evolutionary studies suggest that PRR1 group was the first to diverge and then split the PRR5/9 group and the PRR3/7 group [51]. The early divergence of PRR1 could date back before the divergence of moss from higher plant lineages. PRR1 orthologs in Chlamydomonas reinhardtii, Chlorella variabilis and Ostreococcus tauri [24, 51] supports the hypothesis that the PRR1 orthologs might be the original members of PRR family. In this study, conserved motif analysis revealed that motifs 6 and 9 are present in the PRR5/9 and PRR3/7 groups, but not in the PRR1 group. This finding indicates a distinct divergence between PRR1 group and other PRR groups. Understanding these divergences might provide insights into the functional evolution and specialization of the PRR family in response to environmental adaptations. Recent analysis revealed that PbPRR5/9 and PbPRR3/7 clades appear before differentiation in monocotyledonous and dicotyledonous plants, but the expansion of the two groups happened independently in two types of plants [24]. Analysis of PRR3/7 and PRR5/9 gene expansions using chromosomal synteny suggests that the PRR3/7 clade expansion in monocots is associated with the ρ (rho) polyploidy event, while the PRR5/9 clade duplication happened earlier. In eudicots, the expansion of PRR3/7 and PRR5/9 genes is linked to the γ (gamma) polyploidy event. However, the presence of PRR5/9 genes in water lilies, which diverged before the eudicot-monocot split, indicates that the PRR5/9 duplication in eudicots may have occurred before the γ polyploidy event. The sequence identity and positional orthology suggest that PRR5/9 genes in water lilies are more similar to monocot genes, indicating a complex evolutionary history [24]. In pear genome, PbPRR5/9 clade had two genes as a duplicated gene pair, and PbPRR3/7 clade had four genes that are identified six gene pairs. However, the occurrence time of these gene pairs varied widely, and further understanding the evolutionary history of PRR family in different plants is valuable.

Since plants cannot choose suitable living environment through movement like animals, they must adjust their physiological activities to adapt to periodic changes in the external environment. In Arabidopsis, five PRR genes, as key components of circadian clock, involve in regulating various physiological activities, and their transcription levels oscillate regularly throughout the day [9]. In this study, the expression of eight PbPRR genes had strong diurnal rhythm, which in the same group exhibit a similar pattern. In Arabidopsis, the expression peaks of five PRR genes appear sequentially from morning to evening [17]. The transcription levels of PRR genes in maize show clear diurnal oscillation pattern within 24-h cycle. Starting at dawn, they peaks occur approximately three hours apart, with ZmPRR73, ZmPRR37, ZmPRR95, ZmPRR59, and ZmPRR1 arranged in order of their peak times [27]. However, eight PbPRR genes in pear appeared only two peaks, PbTOC1a and PbTOC1b peaking before dawn (ZT 21), and the remaining six genes peaking at ZT 9. These results speculate that PbPRR genes may have distinctive functions at these phases. The rhythmic feature of circadian clock genes is that they autonomously maintain periodic oscillations under free-running conditions, such as constant light [52]. In addition to PbPRR3, the remaining seven PbPRR genes all have this feature, indicating that they are clock related-genes. Notably, the circadian clock senses changes in the external photoperiod and adjusts itself to synchronize with it [53]. The diurnal expression trend of PbPRR genes has been displayed by analyzing leaf transcriptome data under different photoperiodic conditions [54]. Combining three photoperiods, including 12-h light/12-h dark, 16-h light/8-h dark (long-day) and 8-h light/16-h dark (short-day), we found that the change of light signal had different effects on PbPRR genes. For example, compared with the other two conditions, the peak time of PbTOC1b and PbPRR7a/b/c is significantly earlier under short-day conditions, while the peak time of PbPRR59a/b under long-day conditions is delayed. Similar diurnal patterns have been reported in crops such as maize [27]. Compared with the long-day conditions, the peak time of ZmPRR1-1 and ZmPRR1-2 is three hours earlier under short-day conditions. Different from the effect of photoperiod in pear on the peak time of PRR genes, the expression levels of GmPRRs in soybean under long-day conditions was higher than that under short-day conditions [30]. As clock-related and photoperiod-responsive genes, PbPRR may participate in the cooperative regulation of pear growth and development, and their potential functions need to be further explored.

Various functions of PRR genes in different plants have been identified, including flowering, hypocotyl growth and other developmental processes, as well as response to abiotic stresses such as cold, drought and salt [20, 21, 34, 55,56,57]. ppd-H1 mutant causes late flowering under long-day condition. Ppd-H1 is identified as HvPRR37 in barley, and the expressions of HvCO and HvFT decrease in ppd-H1 mutant [58]. In the past 20 years, similar researches have been reported in rice, sorghum, wheat, soybean, with functional genes clustered in the PRR3/7 clade [35, 37, 38, 59]. These PRR genes in crops exhibit photoperiodic sensitivity and play critical roles in flowering time regulation, leading to alter of yield and growth areas. Based on the pervasive impact of the circadian clock systems on crops, more studies have been devoted to improving agricultural traits by modifying clock-related genes [10]. Therefore, it is of great significance to explore the biological functions of PRR genes in pear, especially in flowering related to fruit. We focused on the performance of PbPRR59a and PbPRR59b genes in flowering regulation. They are highly conserved with AtPRR5, including sequence characteristics, expression patterns, and subcellular localization. AtPRR5 shows opposite regulatory effects in Arabidopsis and rice, promoting flowering of Arabidopsis and delaying flowering of rice [21, 60]. In this study, overexpression of both PbPRR59a and PbPRR59b could inhibit the flowering of transgenic Arabidopsis, indicating that the role of homologous genes in PRR5/9 clade may vary in different species. The current study shows that the complexity of circadian clock network tends to increase during plant evolution. Further studies will elucidate the specific role and molecular mechanism of PbPRR genes in pear flowering, and lay a foundation for the construction of pear circadian clock system.

Conclusions

In this study, 43 PRR genes were identified from seven Rosaceae species, and phylogenetic tree, duplication events and synteny analyses were performed. A more comprehensive analyses, including expression patterns, subcellular localization, and biological functions, were conducted for PbPRR genes. Our findings revealed that PbPRR genes had stable rhythms as clock-related genes. Notably, overexpression of PbPRR59a and PbPRR59b delayed flowering in transgenic Arabidopsis plants. Overall, our results shed light on the involvement of potential pear clock genes PbPRR59a and PbPRR59b in flowering regulation. Circadian clock has great potential and value in agricultural production, and the molecular mechanism of PbPRR genes in regulating pear flowering will be comprehensively and deeply studied in the future, so as to provide the basis for high-quality and efficient pear industry.

Methods

Plants materials

For expression experiments, materials were collected from pear trees (Pyrus bretschneideri cultivar ‘Dangshan Suli’) growing in experimental orchard at Nanjing Agricultural University in Nanjing, China. Leaf buds and flower buds were collected in March. Buds ready for flowering were picked to collect the petals, anthers, and ovaries separately. Seeds used in this study were harvested from pear trees. The sprouted and rooted pear seedlings were cultured in a growth chamber to collect roots, stems and leaves. The ambient condition of the chamber was photoperiod 12-h light/12-h dark, 100 μmol m−2 s−1 light, temperature 22 °C, and 65% relative humidity. Diurnal expression experiment was carried out when pear seedlings grew for 30 days under the same condition. The time when the light turns on is defined as zeitgeber time zero (ZT 0). Under 12-h light/12-h dark conditions, leaf samples were collected at ZT 1, ZT 5, ZT 9, ZT 13, ZT 17, and ZT 21 time points in one day, respectively. There were three replicates at each sampling point, each consisting of three randomly selected seedlings with a total of nine leaves. At the same time, some seedlings were transferred to constant light conditions. Under constant light conditions, leaf samples were collected at each corresponding time point (ZT 1, ZT 5, ZT 9, ZT 13, ZT 17, and ZT 21) for three consecutive days. Each experiment had three biological replicates. All samples were frozen immediately in liquid nitrogen and stored at -80 °C.

Arabidopsis and tobacco (Nicotiana benthamiana) plants were cultured in a similar chamber with photoperiod 16-h light/8-h dark. Murashige and Skoog (MS) medium with hygromycin was used to screen Arabidopsis transgenic seedlings. The statistics of flowering phenotype and gene expression analysis were measured in T3 homozygous transgenic lines.

Gene identification

The genome information of pear (Pyrus bretschneideri) was acquired from the Pear Genome Project (http://gigadb.org/dataset/100083) [44]. The genome information of apple (Malus domestica) and peach (Prunus persica) were acquired from Phytozome (https://phytozome-next.jgi.doe.gov). The genome information of strawberry (Fragaria vesca), black raspberry (Rubus occidentali), and sweet cherry (Prunus avium) were acquired from the Genome Database for Rosaceae (https://www.rosaceae.org/). The genome information of Japanese apricot (Prunus mume) was acquired from the Prunus mume Genome Project [61] (https://github.com/lileiting/prunusmumegenome).

Protein sequences of five PRR members in Arabidopsis (Arabidopsis thaliana) were download from TAIR (http://www.Arabidopsis.org/). To identify the PRRs in the above seven Rosaceae species, AtPRR proteins served as query to perform BLAST in TBtools software with default parameters [62]. The candidate protein sequences were blast in NCBI database to confirm. The redundant and incomplete sequences were manually removed. Basic information of PRR proteins were analyzed using ProtParam online tool (https://web.expasy.org/protparam/), including number of amino acids, molecular weight and theoretical isoelectric point.

Phylogenetic analysis

ClustalW in MEGA7.0 software was used to perform multiple sequence alignment of PRR protein sequences from Arabidopsis and Rosaceae species. Next, the phylogenetic tree of above PRR proteins was constructed by maximum likelihood method in MEGA7.0 software, and the parameters were set to bootstrap value 1000 and Partial deletion 95% [63]. iTOL online tool (Interactive Tree Of Life, https://itol.embl.de/) was used to visualize and annotate the phylogenetic tree [64].

Evolution and synteny analysis

DupGen_finder (https://github.com/qiao-xin/DupGen_finder) was used to identify PRR paralogous gene pairs and corresponding duplication events in the genome of each Rosaceae species [41]. KaKs_caculator 2.0 software combined with Nei-Gojobori method was used to calculate Ka, Ks and ratio of duplicated gene pairs [65]. The synteny analysis between pear and six Rosaceae species was performed according to a method similar to the Plant Genome Duplication Database (http://chibba.agtec.uga.edu/duplication/) [66]. The potential orthologous gene pairs were identified by DIAMOND software [67], and the syntenic chains were identified by MCScanX software [45]. The final syntenic relationships were visualized using TBtools software.

Conserved motif and gene structure analysis

Conserved motifs of PRR proteins were predicted using MEME (Multiple Em for Motif Elicitation) online tool (http://meme-suite.org/tools/meme) [68]. The number of motifs was changed to 10, leaving the other parameters as default. Gene structures of PRR genes were plotted using GSDS (Gene Structure Display Server) online tool (http://gsds.gao-lab.org/) [69]. These results were integrated using TBtools software.

RNA extraction and quantitative real‑time PCR (qRT-PCR)

The Plant Total RNA Isolation Kit (FOREGENE, Chengdu, China) was used to extract total RNA from pear and Arabidopsis frozen tissues [70]. The OneStep gDNA Removal and cDNA Synthesis SuperMix (TransGen Biotech, Beijing, China) was used to reverse transcribe 1 μg total RNA [71]. All operations were performed according to the instructions. qRT-PCR was performed using SYBR Green I Master Mix (Roche, Germany) on a Roche LightCycler 480 II. PbUBQ (POLYUBIQUITIN) was as the internal reference gene for pear and AtACTIN was as the internal reference gene for Arabidopsis. They were applied to calculated relative expression according to the 2−Δct method [71]. Three biological replicates in each experiment were measured. All qRT-PCR experiments followed MIQE guidelines [72]. Gene-specific primers for selected genes are listed in Table S4.

Subcellular localization analysis and plant transformation

The full-length coding sequence of PbPRR59a and PbPRR59b without the termination codon were respectively inserted into pCAMBIA1300 vector, which was driven by the CaMV (cauliflower mosaic virus) 35S promoter and fused with a GFP protein [73]. The recombinant plasmids and empty vector plasmid were respectively transformed into Agrobacterium tumefaciens GV3101 cells, and then injected into tobacco leaves. The subcellular localization assay was performed according to a published protocol [74]. DAPI (Thermo Fisher Scientific, US) is a nucleic acid stain to visualize nuclei. The fluorescence in tobacco epidermal cells was detected with a confocal laser scanning microscope LSM800 (Zeiss, Germany). To generate PbPRR59a and PbPRR59b overexpression transgenic plants, the corresponding Agrobacterium strains were transformed into Arabidopsis accession Columbia (Col-0) using the floral dip method [75]. The empty vector was also transformed into Arabidopsis Col-0 as the control plant. All transgenic lines were screened on MS medium containing hygromycin, and confirmed by semi-quantitative RT-PCR analysis with primers shown in Table S4.

Availability of data and materials

All data used in this study are included in this article and additional flies. All genome sequence used in this study are publicly available in: Arabidopsis (http://www.Arabidopsis.org/), Chinese white pear (http://gigadb.org/dataset/100083), apple and peach (https://phytozome-next.jgi.doe.gov), strawberry, black raspberry and sweet cherry (https://www.rosaceae.org/), Japanese apricot (https://github.com/lileiting/prunusmumegenome).

Abbreviations

PRR:

PSEUDO RESPONSE REGULATOR

CCA1:

CIRCADIAN CLOCK ASSOCIATED 1

LHY:

LATE ELONGATED HYPOCOTYL

ELF3:

EARLY FLOWERING 3

LUX:

LUX ARRHYTHMO

TOC1:

TIMING OF CAB EXPRESSION 1

CO:

CONSTANS

BTC1:

BOLTING TIME CONTROL 1

GI:

GIGANTEA

psREC:

pseudo receiver

CCT:

CONSTANS, CO-like, and TOC1

FT:

FLOWERING LOCUS T

DSD:

dispersed duplication

WGD:

whole-genome duplication

TD:

tandem duplication

TRD:

transposed duplication

PD:

proximal duplication

ZT:

zeitgeber time

GFP:

green fluorescent protein

OE:

overexpression

qRT-PCR:

quantitative real-time PCR

References

  1. Xu X, Yuan L, Yang X, Zhang X, Wang L, Xie Q. Circadian clock in plants: Linking timing to fitness. J Integr Plant Biol. 2022;64(4):792–811.

    Article  CAS  PubMed  Google Scholar 

  2. Sanchez SE, Kay SA. The plant circadian clock: From a simple timekeeper to a complex developmental manager. Cold Spring Harb Perspect Biol. 2016;8(12): a027748.

    Article  PubMed  PubMed Central  Google Scholar 

  3. Xu X, Yuan L, Xie Q. The circadian clock ticks in plant stress responses. Stress Biol. 2022;2(1):15.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  4. Muroya M, Oshima H, Kobayashi S, Miura A, Miyamura Y, Shiota H, et al. Circadian Clock in Arabidopsis thaliana Determines Flower Opening Time Early in the Morning and Dominantly Closes Early in the Afternoon. Plant Cell Physiol. 2021;62(5):883–93.

    Article  CAS  PubMed  Google Scholar 

  5. Song YH, Shim JS, Kinmonth-Schultz HA, Imaizumi T. Photoperiodic flowering: time measurement mechanisms in leaves. Annu Rev Plant Biol. 2015;66:441–64.

    Article  CAS  PubMed  Google Scholar 

  6. Dodd AN, Kusakina J, Hall A, Gould PD, Hanaoka M. The circadian regulation of photosynthesis. Photosynth Res. 2014;119(1–2):181–90.

    Article  CAS  PubMed  Google Scholar 

  7. Nusinow DA, Helfer A, Hamilton EE, King JJ, Imaizumi T, Schultz TF, et al. The ELF4-ELF3-LUX complex links the circadian clock to diurnal control of hypocotyl growth. Nature. 2011;475(7356):398–402.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  8. Hotta CT, Gardner MJ, Hubbard KE, Baek SJ, Dalchau N, Suhita D, et al. Modulation of environmental responses of plants by circadian clocks. Plant Cell Environ. 2007;30(3):333–49.

    Article  CAS  PubMed  Google Scholar 

  9. Nohales MA, Kay SA. Molecular mechanisms at the core of the plant circadian oscillator. Nat Struct Mol Biol. 2016;23(12):1061–9.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  10. Steed G, Ramirez DC, Hannah MA, Webb AAR. Chronoculture, harnessing the circadian clock to improve crop yield and sustainability. Science. 2021;372(6541):eabc9141.

    Article  CAS  PubMed  Google Scholar 

  11. Bendix C, Marshall CM, Harmon FG. Circadian Clock Genes Universally Control Key Agricultural Traits. Mol Plant. 2015;8(8):1135–52.

    Article  CAS  PubMed  Google Scholar 

  12. Millar A, Carre I, Strayer C, Chua N, Kay S. Circadian clock mutants in Arabidopsis identified by luciferase imaging. Science. 1995;267(5201):1161–3.

    Article  CAS  PubMed  Google Scholar 

  13. Alabadi D, Oyama T, Yanovsky MJ, Harmon FG, Mas P, Kay SA. Reciprocal regulation between TOC1 and LHY/CCA1 within the Arabidopsis circadian clock. Science. 2001;293(5531):880–3.

    Article  CAS  PubMed  Google Scholar 

  14. Para A, Farre EM, Imaizumi T, Pruneda-Paz JL, Harmon FG, Kay SA. PRR3 Is a vascular regulator of TOC1 stability in the Arabidopsis circadian clock. Plant Cell. 2007;19(11):3462–73.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  15. Nakamichi N, Kita M, Ito S, Sato E, Yamashino T, Mizuno T. The Arabidopsis pseudo-response regulators, PRR5 and PRR7, coordinately play essential roles for circadian clock function. Plant Cell Physiol. 2005;46(4):609–19.

    Article  CAS  PubMed  Google Scholar 

  16. Farre EM, Harmer SL, Harmon FG, Yanovsky MJ, Kay SA. Overlapping and distinct roles of PRR7 and PRR9 in the Arabidopsis circadian clock. Curr Biol. 2005;15(1):47–54.

    Article  CAS  PubMed  Google Scholar 

  17. Matsushika A, Makino S, Kojima M, Mizuno T. Circadian waves of expression of the APRR1/TOC1 family of pseudo-response regulators in Arabidopsis thaliana: insight into the plant circadian clock. Plant Cell Physiol. 2000;41(9):1002–12.

    Article  CAS  PubMed  Google Scholar 

  18. Liu T, Carlsson J, Takeuchi T, Newton L, Farre EM. Direct regulation of abiotic responses by the Arabidopsis circadian clock component PRR7. Plant J. 2013;76(1):101–14.

    Article  CAS  PubMed  Google Scholar 

  19. Nakamichi N, Kusano M, Fukushima A, Kita M, Ito S, Yamashino T, et al. Transcript profiling of an Arabidopsis PSEUDO RESPONSE REGULATOR arrhythmic triple mutant reveals a role for the circadian clock in cold stress response. Plant Cell Physiol. 2009;50(3):447–62.

    Article  CAS  PubMed  Google Scholar 

  20. Fukushima A, Kusano M, Nakamichi N, Kobayashi M, Hayashi N, Sakakibara H, et al. Impact of clock-associated Arabidopsis pseudo-response regulators in metabolic coordination. Proc Natl Acad Sci U S A. 2009;106(17):7251–6.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  21. Nakamichi N, Kita M, Niinuma K, Ito S, Yamashino T, Mizoguchi T, et al. Arabidopsis clock-associated pseudo-response regulators PRR9, PRR7 and PRR5 coordinately and positively regulate flowering time through the canonical CONSTANS-dependent photoperiodic pathway. Plant Cell Physiol. 2007;48(6):822–32.

    Article  CAS  PubMed  Google Scholar 

  22. Shim JS, Kubota A, Imaizumi T. Circadian Clock and Photoperiodic Flowering in Arabidopsis: CONSTANS Is a Hub for Signal Integration. Plant Physiol. 2017;173(1):5–15.

    Article  CAS  PubMed  Google Scholar 

  23. Hayama R, Sarid-Krebs L, Richter R, Fernandez V, Jang S, Coupland G. PSEUDO RESPONSE REGULATORs stabilize CONSTANS protein to promote flowering in response to day length. EMBO J. 2017;36(7):904–18.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  24. Hotta CT. The evolution and function of the PSEUDO RESPONSE REGULATOR gene family in the plant circadian clock. Genet Mol Biol. 2022;45: e20220137.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  25. Farre EM, Liu T. The PRR family of transcriptional regulators reflects the complexity and evolution of plant circadian clocks. Curr Opin Plant Biol. 2013;16(5):621–9.

    Article  CAS  PubMed  Google Scholar 

  26. Murakami M, Matsushika A, Ashikari M, Yamashino T, Mizuno T. Circadian-associated rice pseudo response regulators (OsPRRs): insight into the control of flowering time. Biosci Biotechnol Biochem. 2005;69(2):410–4.

    Article  CAS  PubMed  Google Scholar 

  27. Wang C, Wang L, Liu Q, Zhang Y, Dong K. Genome-Wide Identification and Characterization of PRR Gene Family and their Diurnal Rhythmic Expression Profile in Maize. Int J Genomics. 2022;2022:6941607.

    Article  PubMed  PubMed Central  Google Scholar 

  28. Errum A, Rehman N, Khan MR, Ali GM. Genome-wide characterization and expression analysis of pseudo-response regulator gene family in wheat. Mol Biol Rep. 2021;48(3):2411–27.

    Article  CAS  PubMed  Google Scholar 

  29. Wang J, Du Z, Huo X, Zhou J, Chen Y, Zhang J, et al. Genome-wide analysis of PRR gene family uncovers their roles in circadian rhythmic changes and response to drought stress in Gossypium hirsutum L. PeerJ. 2020;8: e9936.

    Article  PubMed  PubMed Central  Google Scholar 

  30. Wang P, Wang L, Zhang L, Wu T, Sun B, Zhang J, et al. Genomic Dissection and Diurnal Expression Analysis Reveal the Essential Roles of the PRR Gene Family in Geographical Adaptation of Soybean. Int J Mol Sci. 2022;23(17):9970.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  31. Jalal A, Sun J, Chen Y, Fan C, Liu J, Wang C. Evolutionary Analysis and Functional Identification of Clock-Associated PSEUDO-RESPONSE REGULATOR (PRRs) Genes in the Flowering Regulation of Roses. Int J Mol Sci. 2022;23(13):7335.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  32. Wang S, Zhang C, Zhao J, Li R, Lv J. Expression analysis of four pseudo-response regulator (PRR) genes in Chrysanthemum morifolium under different photoperiods. PeerJ. 2019;7: e6420.

    Article  PubMed  PubMed Central  Google Scholar 

  33. Dally N, Xiao K, Holtgrawe D, Jung C. The B2 flowering time locus of beet encodes a zinc finger transcription factor. Proc Natl Acad Sci U S A. 2014;111(28):10365–70.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  34. Pin PA, Zhang W, Vogt SH, Dally N, Büttner B, Schulze-Buxloh G, et al. The role of a pseudo-response regulator gene in life cycle adaptation and domestication of beet. Curr Biol. 2012;22(12):1095–101.

    Article  CAS  PubMed  Google Scholar 

  35. Lu S, Dong L, Fang C, Liu S, Kong L, Cheng Q, et al. Stepwise selection on homeologous PRR genes controlling flowering and maturity during soybean domestication. Nat Genet. 2020;52(4):428–36.

    Article  CAS  PubMed  Google Scholar 

  36. Li C, Li YH, Li Y, Lu H, Hong H, Tian Y, et al. A domestication-associated gene GmPRR3b regulates the circadian clock and flowering time in soybean. Mol Plant. 2020;13(5):745–59.

    Article  CAS  PubMed  Google Scholar 

  37. Koo BH, Yoo SC, Park JW, Kwon CT, Lee BD, An G, et al. Natural variation in OsPRR37 regulates heading date and contributes to rice cultivation at a wide range of latitudes. Mol Plant. 2013;6(6):1877–88.

    Article  CAS  PubMed  Google Scholar 

  38. Murphy RL, Klein RR, Morishige DT, Brady JA, Rooney WL, Miller FR, et al. Coincident light and clock regulation of pseudoresponse regulator protein 37 (PRR37) controls photoperiodic flowering in sorghum. Proc Natl Acad Sci U S A. 2011;108(39):16469–74.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  39. Campoli CSM, Davis SJ, von Korff M. Expression conservation within the circadian clock of a monocot: natural variation at barley Ppd-H1 affects circadian expression of flowering time genes, but not clock orthologs. BMC Plant Biol. 2012;12:97.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  40. Panchy N, Lehti-Shiu M, Shiu SH. Evolution of Gene Duplication in Plants. Plant Physiol. 2016;171(4):2294–316.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  41. Qiao X, Li Q, Yin H, Qi K, Li L, Wang R, et al. Gene duplication and evolution in recurring polyploidization-diploidization cycles in plants. Genome Biol. 2019;20(1):38.

    Article  PubMed  PubMed Central  Google Scholar 

  42. Qiao X, Yin H, Li L, Wang R, Wu J, Wu J, et al. Different modes of gene duplication show divergent evolutionary patterns and contribute differently to the expansion of gene families involved in important fruit traits in pear (Pyrus bretschneideri). Front Plant Sci. 2018;9:161.

    Article  PubMed  PubMed Central  Google Scholar 

  43. Blanc G, Wolfe KH. Widespread paleopolyploidy in model plant species inferred from age distributions of duplicate genes. Plant Cell. 2004;16(7):1667–78.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  44. Wu J, Wang Z, Shi Z, Zhang S, Ming R, Zhu S, et al. The genome of the pear (Pyrus bretschneideri Rehd.). Genome Res. 2013;23(2):396–408.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  45. Wang Y, Tang H, Debarry JD, Tan X, Li J, Wang X, et al. MCScanX: a toolkit for detection and evolutionary analysis of gene synteny and collinearity. Nucleic Acids Res. 2012;40(7): e49.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  46. Kaczorowski KA, Quail PH. Arabidopsis PSEUDO-RESPONSE REGULATOR7 Is a signaling intermediate in phytochrome-regulated seedling deetiolation and phasing of the circadian clock. Plant Cell. 2003;15(11):2654–65.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  47. Liu H, Zhou X, Li Q, Wang L, Xing Y. CCT domain-containing genes in cereal crops: flowering time and beyond. Theor Appl Genet. 2020;133(5):1385–96.

    Article  CAS  PubMed  Google Scholar 

  48. Li Y, Yu S, Zhang Q, Wang Z, Liu M, Zhang A, et al. Genome-Wide Identification and Characterization of the CCT Gene Family in Foxtail Millet (Setaria italica) Response to Diurnal Rhythm and Abiotic Stress. Genes (Basel). 2022;13(10):1829.

    Article  CAS  PubMed  Google Scholar 

  49. Linde AM, Eklund DM, Kubota A, Pederson ERA, Holm K, Gyllenstrand N, et al. Early evolution of the land plant circadian clock. New Phytol. 2017;216(2):576–90.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  50. Johansson M, Ibanez C, Takata N, Eriksson ME. The perennial clock is an essential timer for seasonal growth events and cold hardiness. Methods Mol Biol. 2014;1158:297–311.

    Article  PubMed  Google Scholar 

  51. Satbhai SB, Yamashino T, Okada R, Nomoto Y, Mizuno T, Tezuka Y, et al. Pseudo-response regulator (PRR) homologues of the moss Physcomitrella patens: insights into the evolution of the PRR family in land plants. DNA Res. 2011;18(1):39–52.

    Article  CAS  PubMed  Google Scholar 

  52. Harmer SL. The circadian system in higher plants. Annu Rev Plant Biol. 2009;60:357–77.

    Article  CAS  PubMed  Google Scholar 

  53. Creux N, Harmer S. Circadian Rhythms in Plants. Cold Spring Harb Perspect Biol. 2019;11(9): a034611.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  54. Liu Z, Liu W, Wang Z, Qi K, Xie Z, Zhang S, et al. Diurnal transcriptome dynamics reveal the photoperiod response of Pyrus. Physiol Plant. 2023;175(2): e13893.

    Article  CAS  PubMed  Google Scholar 

  55. Wei H, Wang X, He Y, Xu H, Wang L. Clock component OsPRR73 positively regulates rice salt tolerance by modulating OsHKT2;1-mediated sodium homeostasis. EMBO J. 2021;40(3): e105086.

    Article  CAS  PubMed  Google Scholar 

  56. Li N, Zhang Y, He Y, Wang Y, Wang L. Pseudo Response Regulators Regulate Photoperiodic Hypocotyl Growth by Repressing PIF4/5 Transcription. Plant Physiol. 2020;183(2):686–99.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  57. Nakamichi N, Takao S, Kudo T, Kiba T, Wang Y, Kinoshita T, et al. Improvement of Arabidopsis Biomass and Cold, Drought and Salinity Stress Tolerance by Modified Circadian Clock-Associated PSEUDO-RESPONSE REGULATORs. Plant Cell Physiol. 2016;57(5):1085–97.

    Article  CAS  PubMed  Google Scholar 

  58. Turner A, Beales J, Faure S, Dunford RP, Laurie DA. The pseudo-response regulator Ppd-H1 provides adaptation to photoperiod in barley. Science. 2005;310(5750):1031–4.

    Article  CAS  PubMed  Google Scholar 

  59. Beales J, Turner A, Griffiths S, Snape JW, Laurie DA. A pseudo-response regulator is misexpressed in the photoperiod insensitive Ppd-D1a mutant of wheat (Triticum aestivum L.). Theor Appl Genet. 2007;15(5):721–33.

    Article  Google Scholar 

  60. Nakamichi N, Kudo T, Makita N, Kiba T, Kinoshita T, Sakakibara H. Flowering time control in rice by introducing Arabidopsis clock-associated PSEUDO-RESPONSE REGULATOR 5. Biosci Biotechnol Biochem. 2020;84(5):970–9.

    Article  CAS  PubMed  Google Scholar 

  61. Zhang Q, Chen W, Sun L, Zhao F, Huang B, Yang W, et al. The genome of Prunus mume. Nat Commun. 2012;3:1318.

    Article  PubMed  Google Scholar 

  62. Chen C, Chen H, Zhang Y, Thomas HR, Frank MH, He Y, et al. TBtools: an integrative toolkit developed for interactive analyses of big biological data. Mol Plant. 2020;13(8):1194–202.

    Article  CAS  PubMed  Google Scholar 

  63. Kumar S, Stecher G, Tamura K. MEGA7: Molecular evolutionary genetics analysis version 7.0 for bigger datasets. Mol Biol Evol. 2016;33(7):1870–4.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  64. Letunic I, Bork P. Interactive Tree Of Life (iTOL) v5: an online tool for phylogenetic tree display and annotation. Nucleic Acids Res. 2021;49(W1):W293–6.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  65. Wang D, Zhang Y, Zhang Z, Zhu J, Yu J. KaKs_Calculator 2.0: a toolkit incorporating gamma-series methods and sliding window strategies. Genom Proteom Bioinf. 2010;8(1):77–80.

    Article  CAS  Google Scholar 

  66. Lee TH, Tang H, Wang X, Paterson AH. PGDD: a database of gene and genome duplication in plants. Nucleic Acids Res. 2013;41(Database issue):D1152-1158.

    CAS  PubMed  Google Scholar 

  67. Buchfink B, Xie C, Huson DH. Fast and sensitive protein alignment using DIAMOND. Nat Methods. 2015;12(1):59–60.

    Article  CAS  PubMed  Google Scholar 

  68. Bailey TL, Williams N, Misleh C, Li WW. MEME: discovering and analyzing DNA and protein sequence motifs. Nucleic Acids Res. 2006;34:W369-373.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  69. Hu B, Jin J, Guo AY, Zhang H, Luo J, Gao G. GSDS 2.0: an upgraded gene feature visualization server. Bioinformatics. 2015;31(8):1296–7.

    Article  PubMed  Google Scholar 

  70. Wang P, Li Y, Liu Z, Li X, Wang Y, Liu W, et al. Reciprocal regulation of flower induction by ELF3alpha and ELF3beta generated via alternative promoter usage. Plant Cell. 2023;35(6):2095–113.

    Article  PubMed  PubMed Central  Google Scholar 

  71. Liu Z, Zhu X, Liu W, Qi K, Xie Z, Zhang S, et al. Characterization of the REVEILLE family in Rosaceae and role of PbLHY in flowering time regulation. BMC Genomics. 2023;24(1):49.

    Article  PubMed  PubMed Central  Google Scholar 

  72. Bustin SA, Benes V, Garson JA, Hellemans J, Huggett J, Kubista M, et al. The MIQE guidelines: minimum information for publication of quantitative real-time PCR experiments. Clin Chem. 2009;55(4):611–22.

    Article  CAS  PubMed  Google Scholar 

  73. Xie Q, Wang P, Liu X, Yuan L, Wang L, Zhang C, et al. LNK1 and LNK2 are transcriptional coactivators in the Arabidopsis circadian oscillator. Plant Cell. 2014;26(7):2843–57.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  74. Sparkes IA, Runions J, Kearns A, Hawes C. Rapid, transient expression of fluorescent fusion proteins in tobacco plants and generation of stably transformed plants. Nat Protoc. 2006;1(4):2019–25.

    Article  CAS  PubMed  Google Scholar 

  75. Clough SJ, Bent AF. Floral dip: a simplified method for Agrobacterium-mediated transformation of Arabidopsis thaliana. Plant J. 1998;16(6):735–43.

    Article  CAS  PubMed  Google Scholar 

Download references

Acknowledgements

We thank the Bioinformatics Center of Nanjing Agricultural University for supporting bioinformatic analysis. We thank Dr. Yuehua Ma (Central laboratory of College of Horticulture, Nanjing Agricultural University) for assistance in using laser scanning confocal microscope LSM800.

Funding

This work is supported by Fundamental Research Program of Shanxi Province (20210302124231); the National Natural Science Foundation of China (32302515); Natural Science Foundation of Jiangsu Province (BK20221012); National Key Laboratory for Germplasm Innovation & Utilization of Horticultural Crops (Horti-KF-2023–05), Ningbo Key Laboratory of Characteristic Horticultural Crops in Quality Adjustment and Resistance Breeding (NBYYL2023001), Earmarked Fund for XJARS (XJLGCYJSTX05-2024–07), Tianshan Talents Program of Xinjiang (2023D14015), Priority Academic Program Development of Jiangsu Higher Education Institutions, and Earmarked Fund for China Agriculture Research System (CARS-28).

Author information

Author notes

  1. Zhe Liu and Weijuan Liu contributed equally to this work.

Authors and Affiliations

  1. School of Pharmacy, Changzhi Medical College, Changzhi, 046000, China

    Zhe Liu

  2. Sanya Institute of Nanjing Agricultural University, State Key Laboratory of Crop Genetics & Germplasm Enhancement and Utilization, Jiangsu Key Laboratory for Horticultural Crop Breeding, College of Horticulture, Nanjing Agricultural University, Nanjing, 210095, China

    Zhe Liu, Weijuan Liu, Zhangqing Wang, Zhihua Xie, Kaijie Qi, Dong Yue, Yu Li, Shaoling Zhang, Juyou Wu & Peng Wang

  3. Zhongshan Biological Breeding Laboratory, Nanjing, 210014, China

    Juyou Wu

Authors
  1. Zhe Liu
    View author publications

    You can also search for this author in PubMed Google Scholar

  2. Weijuan Liu
    View author publications

    You can also search for this author in PubMed Google Scholar

  3. Zhangqing Wang
    View author publications

    You can also search for this author in PubMed Google Scholar

  4. Zhihua Xie
    View author publications

    You can also search for this author in PubMed Google Scholar

  5. Kaijie Qi
    View author publications

    You can also search for this author in PubMed Google Scholar

  6. Dong Yue
    View author publications

    You can also search for this author in PubMed Google Scholar

  7. Yu Li
    View author publications

    You can also search for this author in PubMed Google Scholar

  8. Shaoling Zhang
    View author publications

    You can also search for this author in PubMed Google Scholar

  9. Juyou Wu
    View author publications

    You can also search for this author in PubMed Google Scholar

  10. Peng Wang
    View author publications

    You can also search for this author in PubMed Google Scholar

Contributions

All authors contributed to the research planning and experimental designs; P. W., J. W., S. Z. initiated and supervised the project; Z. L., W. L., Z. W., K. Q., Z. X., D. Y., and Y. L. performed the experiments and analyzed the data; Z. L. and P. W. wrote the manuscript. All authors read and approved the manuscript.

Corresponding author

Correspondence to Peng Wang.

Ethics declarations

Ethics approval and consent to participate

All methods in this research were carried out in accordance with relevant guidelines. No specific permits are required for sample collection in this study.

Consent for publication

Not applicable.

Competing interests

The authors declare no competing interests.

Additional information

Publisher’s Note

Springer Nature remains neutral with regard to jurisdictional claims in published maps and institutional affiliations.

Supplementary Information

12864_2024_10720_MOESM1_ESM.xlsx

Supplementary Material 1: Table S1. Characteristics of the PRR family members in the seven Rosaceae species. Table S2 Numbers of PRR gene pairs from different duplication events in seven Rosaceae species. Table S3 Nonsynonymous substitution rates (Ka) and synonymous substitution rates (Ks) calculation of duplicated PRR gene pairs in seven Rosaceae species. Table S4 The primers used in the assays.

12864_2024_10720_MOESM2_ESM.pdf

Supplementary Material 2: Fig. S1. Original gels for Fig. 9b. The red rectangular box represents the cropped gels.

Rights and permissions

Open Access This article is licensed under a Creative Commons Attribution-NonCommercial-NoDerivatives 4.0 International License, which permits any non-commercial use, sharing, distribution and reproduction in any medium or format, as long as you give appropriate credit to the original author(s) and the source, provide a link to the Creative Commons licence, and indicate if you modified the licensed material. You do not have permission under this licence to share adapted material derived from this article or parts of it. The images or other third party material in this article are included in the article’s Creative Commons licence, unless indicated otherwise in a credit line to the material. If material is not included in the article’s Creative Commons licence and your intended use is not permitted by statutory regulation or exceeds the permitted use, you will need to obtain permission directly from the copyright holder. To view a copy of this licence, visit http://creativecommons.org/licenses/by-nc-nd/4.0/.

Reprints and permissions

About this article

Check for updates. Verify currency and authenticity via CrossMark

Cite this article

Liu, Z., Liu, W., Wang, Z. et al. Molecular characterization of PSEUDO RESPONSE REGULATOR family in Rosaceae and function of PbPRR59a and PbPRR59b in flowering regulation. BMC Genomics 25, 794 (2024). https://doi.org/10.1186/s12864-024-10720-5

Download citation

  • Received:

  • Accepted:

  • Published:

  • DOI: https://doi.org/10.1186/s12864-024-10720-5

Keywords

BMC Genomics

ISSN: 1471-2164

Contact us