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Article

Phloem-Mobile MYB44 Negatively Regulates Expression of PHOSPHATE TRANSPORTER 1 in Arabidopsis Roots

by
Toluwase Olukayode
1,2,
Jieyu Chen
1,
Yang Zhao
1,
Chuanhezi Quan
1,2,
Leon V. Kochian
1,3 and
Byung-Kook Ham
1,2,*
1
Global Institute for Food Security (GIFS), University of Saskatchewan, 421 Downey Rd, Saskatoon, SK S7N 4L8, Canada
2
Department of Biology, University of Saskatchewan, 112 Science Place, Saskatoon, SK S7N 5E2, Canada
3
Department of Plant Science, University of Saskatchewan, 51 Campus Drive, Saskatoon, SK S7N 5A8, Canada
*
Author to whom correspondence should be addressed.
Plants 2023, 12(20), 3617; https://doi.org/10.3390/plants12203617
Submission received: 12 August 2023 / Revised: 3 October 2023 / Accepted: 17 October 2023 / Published: 19 October 2023
(This article belongs to the Special Issue Long Distance Signaling in Plants)
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Abstract

:
Phosphorus (P) is an essential plant macronutrient; however, its availability is often limited in soils. Plants have evolved complex mechanisms for efficient phosphate (Pi) absorption, which are responsive to changes in external and internal Pi concentration, and orchestrated through local and systemic responses. To explore these systemic Pi responses, here we identified AtMYB44 as a phloem-mobile mRNA, an Arabidopsis homolog of Cucumis sativus MYB44, that is responsive to the Pi-starvation stress. qRT-PCR assays revealed that AtMYB44 was up-regulated and expressed in both shoot and root in response to Pi-starvation stress. The atmyb44 mutant displayed higher shoot and root biomass compared to wild-type plants, under Pi-starvation conditions. Interestingly, the expression of PHOSPHATE TRANSPORTER1;2 (PHT1;2) and PHT1;4 was enhanced in atmyb44 in response to a Pi-starvation treatment. A split-root assay showed that AtMYB44 expression was systemically regulated under Pi-starvation conditions, and in atmyb44, systemic controls on PHT1;2 and PHT1;4 expression were moderately disrupted. Heterografting assays confirmed graft transmission of AtMYB44 transcripts, and PHT1;2 and PHT1;4 expression was decreased in heterografted atmyb44 rootstocks. Taken together, our findings support the hypothesis that mobile AtMYB44 mRNA serves as a long-distance Pi response signal, which negatively regulates Pi transport and utilization in Arabidopsis.

1. Introduction

Phosphorus (P) is an essential element that is involved in various functionalities in living organisms, including plants. Therefore, it is critical to ensure proper phosphorus nutrition for optimal plant growth and development, by supplying phosphate (Pi) fertilizers to maximize crop productivity in modern agriculture systems [1,2]. However, soil-applied Pi fertilizer becomes rapidly immobilized, due to chemical reactions with cations (e.g., magnesium, calcium, aluminum, and iron) in both alkaline and acidic soils [3,4]. This can limit the availability of applied Pi to the plant to around 20–30% for plant use [3,4]. Furthermore, Pi is a finite and non-renewable resource; this has led to increased interest in understanding the mechanisms by which plants absorb and use Pi under limiting Pi conditions. Here, the goal is to develop elite plant lines with enhanced P acquisition and utilization efficiency traits [3,4,5,6,7].
Plants have evolved sophisticated adaptative mechanisms, which involve a range of physiological, morphological, biochemical, and molecular processes, to respond to low Pi conditions for efficient Pi foraging in soils [4,5,8,9,10,11]. These adaptative processes, known as phosphate starvation responses (PSRs), are categorized into local and systemic Pi responses as Pi sensing and long-distance signaling, and the adaptative efficiency can be determined by the PSR regulatory capacity in plants [6,10,12,13].
The local Pi responses are largely associated with traits for root growth, as they perceive the Pi level in the soil and determine the root developmental fate in response to the imposed Pi-starvation stress, whereas internal Pi concentration activates the systemic responses to integrate the Pi level information in distantly located plant tissues/organs [6,10,12,13]. Systemic Pi responses play an important role in global P homeostasis within plants, and microRNA399 (miR399) was the first identified long-distance regulatory component in Pi-stress signaling [14,15]. Under Pi-starvation conditions, miR399 is expressed in shoots and delivered into roots via the phloem to mediate the degradation of PHO2 mRNA, which encodes an E2 ubiquitin-conjugating enzyme and regulates the level of high-affinity PHOSTPHATE TRANSPORTER1 (PHT1) protein in roots. Therefore, this systemic regulatory mechanism serves to control Pi acquisition under Pi-starvation stress conditions [6,14,15,16,17,18,19,20].
MYB transcription factors (TFs), one of the largest TF families in plants, contain a conserved DNA-binding domain and up to three tandem repeats of helix-turn-helix domains, designated R1, R2 and R3 [21,22,23]. In plants, MYB44, classified as a member of the R2R3-type MYB subfamily, has been characterized as a regulatory factor in various abiotic and biotic stress responses [24,25,26,27,28]. It was earlier reported that MYB TFs are involved in the control of Pi-starvation responses in plants [28,29,30,31,32,33,34]. PHOSPHATE STARVATION RESPONSE1 (PHR1) is a MYB-related TF, a key regulator in Pi-starvation responses [29]. Arabidopsis MYB62, induced in response to Pi-stress, appears to function as a negative regulator for PSR gene expression and is involved in gibberellic acid biosynthesis [31]. Another MYB-like TF, REGULATOR OF LEAF INCLINATION 1 (RLI1), interacts with SPX1 (Syg1/Pho81/XPR1), and the SPX1-RLI1 complex appears to block RLI1 binding to the promoter regions of RLI1 target genes, which are involved in elongation of leaf cells in the lamina joint in rice [33,34]. Additionally, potato MYB44 functions as a negative regulator of PHOSPHATE1 (PHO1) expression, which encodes a major Pi transport protein that mediates Pi transport from the root to the shoot, through Pi loading into the xylem [28]. However, it remains unknown whether MYB44 plays a role in systemic Pi responses. In this study, Arabidopsis MYB44, referred to as AtMYB44, was characterized as a phloem-mobile mRNA, and shown to be involved in systemic regulation of PHT1 (Pi transporter) gene expression in roots under Pi-starvation conditions. We propose that mobile AtMYB44 mRNA acts as a negative regulator in systemic Pi responses for control of Pi acquisition in Arabidopsis roots.

2. Results

2.1. Identification of Mobile CsMYB44 Orthologs in Arabidopsis

In a previous study, cucumber was used as a model plant to examine the role of the phloem in systemic signaling under Pi-stress conditions [35]. The phloem mRNA profiles changed dynamically, in response to an imposed Pi-stress treatment, and a range of graft-transmissible mRNAs were shown to target specific sink organs/tissues under Pi-stress conditions [35]. The Cucumis sativus MYB44 (CsMYB44, Csa6G491690), encoding an R2R3 MYB transcription factor (TF), was among these Pi-stress-induced graft-transmissible mRNAs and was delivered into sink tissue during the early stage of Pi-stress treatment [35]. Interestingly, even though 112 MYB family members were identified in cucumber, [36] and one specific clade included four other cucumber MYBs with CsMYB44 (Figure S1A), CsMYB44 (Csa6G491690) was detected as the only Pi-stress-responsive mobile mRNA, encoding for a MYB transcription factor [35]. Based on our findings, we hypothesize that mobile CsMYB44 mRNA could serve as an early, long-distance signaling factor for systemic Pi responses. Thus, we selected CsMYB44 to further assess its role as a long-distance signaling mRNA in response to Pi-stress.
First, to facilitate the testing of our hypothesis that MYB44 plays a role in phloem-mediated systemic signaling under Pi-starvation stress conditions, we conducted a phylogenetic analysis to identify putative CsMYB44 orthologs in Arabidopsis. A total of 132 Arabidopsis R2R3 MYB family members were analyzed (Figure S1B), and here, the phylogenetic tree analysis revealed the presence of CsMYB44 in a specific MYB subfamily subclade (Figure 1A and Figure S1). AtMYB77, AtMYB73 and AtMYB70 shared an amino acid sequence identity of 69.0%, 59.5% and 57.8%, respectively, with AtMYB44.
To gain insight into the regulation of the genes in this MYB subclade, we used the Arabidopsis cis-regulatory element database (https://agris-knowledgebase.org/AtcisDB; accessed on 4 February 2020) to analyze the promoter regions of AtMYB44, AtMYB70, AtMYB73 and AtMYB77 with the aim to identify potential cis-elements that might serve to control their expression under Pi-stress conditions. Numerous Pi-starvation responsive (PSR) genes are regulated by PHR1, and the PHR1 binding site (P1BS) is enriched in the promoter regions of many Arabidopsis Pi-responsive genes [37,38,39].
Our cis-element analysis indeed revealed that P1BS motifs were located within the promoters of AtMYB44, AtMYB70 and AtMYB73, but not AtMYB77 (Figure 1B). Furthermore, qRT-PCR analysis established that the transcript levels of AtMYB44, AtMYB70, AtMYB73 and AtMYB77 were responsive to a Pi- stress treatment in both shoots and roots (Figure 1C,D). For AtMYB44 and AtMYB77, at least a two-fold increase and decrease in transcript levels, respectively, were detected in shoots, under Pi-stress conditions (Figure 1C). By contrast, AtMYB70 and AtMYB73 transcript levels in the shoots were only slightly changed in response to Pi-stress (10 µM Pi) (Figure 1C). In roots, the AtMYB44, AtMYB70, AtMYB73 and AtMYB77 transcript levels were significantly increased under Pi-stress conditions (10 µM Pi) (Figure 1D). Taken together, our results demonstrate that the putative CsMYB44 homologs, AtMYB44, AtMYB70, AtMYB73 and AtMYB77, are regulated in response to the imposed Pi-stress treatment. Interestingly, the previous report provided evidence that AtMYB44 and AtMYB70 mRNA were mobile and, in particular, Pi-stress appeared to lead to phloem mobility of AtMYB44 mRNA in Arabidopsis [40]. In addition, AtMYB44 transcript levels increased in both shoot and root (Figure 1C,D); therefore, we focused on investigating the role of AtMYB44 in Pi-stress systemic signaling.

2.2. AtMYB44 Is Expressed in Leaf and Root Vascular Tissues under Pi-Stress Conditions

To further understand the mechanism of AtMYB44 regulation in Arabidopsis, we generated transgenic plants carrying the GFP-GUS reporter under the control of the native AtMYB44 promoter and analyzed the AtMYB44 expression pattern (Figure 2). Consistent with our qRT-PCR results (Figure 1C,D), the β-glucuronidase (GUS) staining assays showed signal in both shoots and roots, and revealed stronger staining under Pi-stress (10 µM) compared with Pi-sufficient conditions (500 µM) (Figure 2A,B), consistent with induction of AtMYB44 expression in response to Pi-stress. Here, AtMYB44 expression was detected in leaf lamina, leaf vasculature, root vasculature, root tips of primary and lateral roots, and in lateral root primordia (Figure 2B–J). Some mature lateral roots also exhibited GUS staining in the vascular tissue of elongation and maturation zones, but not the root tip (Figure 2H, compared with Figure 2G), suggesting that the expression of AtMYB44 would respond to Pi-starvation stress at the lateral root tips. Within the primary root tip, AtMYB44 was highly expressed in the epidermis, cortical layers and endodermis under Pi-starvation conditions (Figure 2K,L). In time-course experiments, the effects of Pi-starvation stress were confirmed on AtMYB44 expression in shoots and roots in Arabidopsis (Figure 2M,N and Figure S2). These findings were consistent with the notion that AtMYB44 plays a role in transcriptional regulation of adaptive shoot and root development in response to Pi-stress treatment.

2.3. AtMYB70, AtMYB73 and AtMYB77 Transcript Levels Were Elevated in atmyb44 Mutant, Compared with Wild-Type

As expression of other AtMYB family genes, close to CsMYB44, was also responsive to imposed Pi-stress (Figure 1D), we hypothesized that other redundant AtMYBs could compensate for the absence of AtMYB44 under Pi-stress conditions. To test this notion, we examined the expression levels of AtMYB70, AtMYB73 and AtMYB77 in the atmyb44 mutant background under Pi-stress conditions using qRT-PCR (Figure 3). Here, we confirmed that the expression of AtMYB70, AtMYB73 and AtMYB77 increased (Figure 3). Enhanced transcript levels of AtMYB70, AtMYB73 and AtMYB77 were detected in atmyb44 plants under both Pi-sufficient and Pi-stress conditions, compared with WT (Figure 3). These assays supported a role for AtMYB70, AtMYB73 and AtMYB77 in the functional compensation of AtMYB44 in its absence.

2.4. The atmyb44 Root Had an Elevated Pi Concentration under Pi-Stress Conditions

Under Pi-sufficient conditions, the atmyb44 mutant exhibited slightly longer primary roots and a higher number of lateral roots, compared with the WT and AtMYB44 overexpression (OX) lines, and, consistent with the previous study [25,41], AtMYB44 overexpression (OX) lines displayed shorter primary roots than WT (Figure S3A–C). However, under Pi-stress conditions, no significant differences in primary root growth were observed between WT, atmyb44 and AtMYB44 OX lines (Figure S3A,B). Interestingly, the lateral root numbers of AtMYB44 OX lines were lower than in WT and atmyb44 mutant lines, and this was observed in both Pi-sufficient and Pi-starvation conditions (Figure S3C). Under Pi-stress conditions, the atmyb44 plants did not exhibit a clear phenotypic difference in primary root growth and lateral root number, compared with WT (Figure S3). As both plant lines were grown on agar medium, which limited observation of plant developmental changes, to apply a prolonged Pi-stress, we next employed a hydroponic system to conduct phenotypic analysis of atmyb44 and AtMYB44 overexpression (OX) lines. In the experiments using the hydroponic system, we reduced the Pi concentration from 10 µM to 5 µM to ensure we were creating effective Pi-starvation treatments in hydroponics, where Pi is more available than in agar growth medium.
Compared to WT, around a 1.2-fold higher and a 1.5-fold lower shoot biomass was observed in the atmyb44 and AtMYB44 OX plants, respectively, under Pi-sufficient conditions, although no significant difference in shoot biomass was detected under Pi-stress conditions (Figure 4A and Figure S4A). However, the root biomass was obviously at least 1.5-fold higher in atmyb44 than WT and AtMYB44 OXs, under both Pi-sufficient and Pi-stress conditions (Figure 4B and Figure S4B). In atmyb44, the Pi concentration was around 2-fold higher in shoots and 1.5-fold lower in roots compared to the level in WT under Pi-sufficient conditions. In contrast, the root Pi concentration in atmyb44 was around 2-fold higher than WT under Pi-stress conditions, even though no significant difference in shoot Pi concentration was detected between WT and atmyb44 (Figure 4C,D). Taken together, these results suggested that AtMYB44 functions as a negative regulator in both shoot and root development under Pi-sufficient conditions and that an absence of AtMYB44 might increase Pi uptake into Arabidopsis roots.

2.5. Expression of PHT1;2 and PHT1;4 Is Negatively Regulated by AtMYB44 in Roots

The in silico analysis using ConnecTF (https://connectf.org; accessed on 23 October 2022) [42] revealed that AtMYB44 could be involved in many gene regulatory pathways and, interestingly, bound to the promoter regions of PHOSPAHTE TRANSPORTER 1;2 (PHT1;2) and PHT1;4 as potential AtMYB44-target sites (Table S2). As we observed an enhanced level of Pi concentration in the root of atmyb44 plants under Pi-stress conditions (Figure 4D), and PHT1 regulates the initial uptake of Pi [6,43,44,45,46,47,48,49,50], we hypothesized that AtMYB44 regulates PHT1 expression in roots for Pi acquisition under Pi-stress conditions.
To test this hypothesis, we examined the expression level of PHT1;2 and PHT1;4 in WT, atmyb44 and AtMYB44 OX-1 roots, using qRT-PCR (Figure 5). The expression levels of PHT1;2 and PHT1;4 were much higher in atmyb44 under Pi-stress conditions compared to WT (two- to four-fold higher expression; Figure 5), and the increased levels of PHT1;2 and PHT1;4 in atmyb44 were diminished in AtMYB44 OX-1 (Figure 5A,B). We did not detect any significant differences in the expression levels of PHT1;2 in AtMYB44 OX-1, compared with WT (Figure 5A). The Type B MONOGALACTOSYL DIACYLGLYCEROL SYNTHASE 3 (MGD3) has been reported as a Pi-starvation response gene [51]; however, it was not predicted to be a AtMYB44 target (Table S2). Compared with the expression patterns of PHT1;2 and PHT1;4, no significant difference in MGD3 expression was observed between WT, atmyb44 and AtMYB44 OX-1 (Figure 5C). It is plausible that AtMYB44 might target the promoter of PHT1;2 and PHT1;4, where it acts as a negative regulator.

2.6. Mobile AtMYB44 mRNA Functions as a Negative Regulator of PHT1;2 and PHT1;4 Expression

We demonstrated that AtMYB44 expression responds to Pi-stress (Figure 1C,D) and AtMYB44 appears to play a role in regulating PHT1;2 and PHT1;4 expression under these conditions (Figure 5). As AtMYB44 was identified as a mobile CsMYB44 ortholog in Arabidopsis (Figure 1A), it is plausible that AtMYB44 could serve as a long-distance signal to exert control over Pi-starvation responses in Arabidopsis. To test whether AtMYB44 acts as a systemic signal in response to Pi-stress, we employed a split-root system to test whether AtMYB44-mediated gene expression is a systemic or local response under Pi-stress conditions. The Arabidopsis root systems grown in the hydroponic culture system were separated into two parts with each half of the root system placed into a vessel containing nutrient solution with Pi (200 µM) or with no Pi (0 µM). As the control, both vessels for each half of the root system on a plant contained the same nutrient solution (CP200 for 200 µM Pi, CP0 for 0 µM) to mimic plant growth under homogenous Pi-sufficient or deficient conditions (Figure 6A) [12].
Total RNA was extracted from these roots for qRT-PCR analysis. First, we investigated regulation of AtMYB44 expression to see if it is part of a systemic response, after Pi-sufficient and deficient treatments were applied to different halves of the root system on individual plants area (Figure 6). As expected, no AtMYB44 transcript was detected in atmyb44 tissues, and AtMYB44 expression in WT was enhanced in response to the imposed Pi-stress (CP0), compared with the mRNA level under Pi-sufficient conditions (CP200) (Figure 6B). In WT, a higher level of AtMYB44 mRNA was detected in that half of a plant’s root system placed in the compartment with 200 µM Pi (SP200), relative to the control (CP200). In addition, lower AtMYB44 mRNA levels were observed for the split root system in 0 µM Pi (SP0) compared to the transcript level in the homogenously Pi-deficient control (CP0) (Figure 6B). These findings support our hypothesis that AtMYB44 serves as a systemic regulator.
Next, we examined systemic regulation of PHT1;2 and PHT1;4 expression in AtMYB44 knockout mutants again using this split-root system to test whether AtMYB44 serves as a factor in systemic PHT1;2 and PHT1;4 regulation. Here, the qRT-PCR analysis revealed that, consistent with the previous report [12], expression of both PHT1;2 and PHT1;4 in WT plants was downregulated in roots within the SP0 container, compared to PHT1;2 and PHT1;4 expression in CP0 in WT (Figure 6C,D). However, in atmyb44 plants, the enhanced transcript levels of PHT1;2 and PHT1;4 were decreased in SP0 compared to CP0 (Figure 6C,D). Taken together, these results suggest that AtMYB44 expression is regulated in a systemic manner, and that other long-distance regulators might be involved in the systemic regulation of PHT1;2 and PHT1;4 regulation in the atmyb44 background.
To investigate whether AtMYB44 mRNA acts as a long-distance regulator for control over PHT1;2 and PHT1;4 expression, we performed micrografting assays between atmyb44 and AtMYB44 OX-1 lines (Figure 7A). Here, our RT-PCR analyses revealed that, as controls, AtMYB44 expression was increased in AtMYB44 OX-1, but not in atmyb44, and AtMYB44 OX-1 and atmyb44 were subsequently used as shoot scions or root stocks (Figure 7B). Analysis of these grafted tissues revealed that the transgene AtMYB44 was detected in rootstocks of heterografted AtMYB44 OX-1 (scion)/atmyb44 (rootstock), but not in the atmyb44 (scion)/ AtMYB44 OX-1 (rootstock), consistent with AtMYB44 mRNA being phloem-mobile from source to sink tissues (Figure 7B). Interestingly, the level of PHT1;2 and PHT1;4 expression was decreased in the rootstocks of these heterografted AtMYB44 OX-1 (scion)/atmyb44 (rootstock) plants, compared to the atmyb44 homograft (Figure 7C). These data support the hypothesis that AtMYB44 mRNA acts as a mobile, negatively acting regulator of PHT1;2 and PHT1;4 expression in Arabidopsis roots.

3. Discussion

The local and systemic regulatory mechanisms acting in Pi acquisition and distribution under Pi-stress conditions have been extensively studied, and many important genes have been identified as crucial components that regulate Pi homeostasis in plants, such as Arabidopsis and rice [4,5,6,29,48,50,52,53]. However, limited information is available on the nature of the systemic Pi-signaling agents that control Pi homeostasis at the whole-plant level [6,14,15,17,35,54,55,56,57]. In this study, we identified AtMYB44 mRNA as a potential mobile systemic Pi-signaling component in Arabidopsis.

3.1. AtMYB44 Expression Responds to an Imposed Pi-Stress

Four homologs of CsMYB44 were identified as potential CsMYB44 orthologs in Arabidopsis (Figure 1A and Figure S1), and their expression patterns were also responsive to an imposed Pi-stress (Figure 1B–D). As the promoter regions of AtMYB44, AtMYB70 and AtMYB73, but not AtMYB77, included PIBS motifs, this suggested that AtMYB44, AtMYB70 and AtMYB73 expression could be regulated in a PHR1-dependent manner under Pi-stress conditions.
An increase in the level of AtMYB44 expression during Pi-starvation treatment and detection of GUS signals within the vascular tissues of both shoot and root (Figure 2) suggested that AtMYB44 could function within the vasculature in response to Pi-starvation stress. In addition, we also observed that AtMYB44 expression was strongly detected in the root tips and lateral root primordia (Figure 2D,G–L). Based on our in silico analysis, the AtMYB44 TF could be associated with the promoter regions of many AUXIN RESPONSE FACTORs (ARFs), which contribute to control over PHR1 expression in Arabidopsis roots under Pi-starvation conditions [58,59] (Table S2). As AtMYB44 expression is responsive to auxin levels in the root [60], AtMYB44 may participate in auxin-dependent root development in response to Pi-stress.
AtMYB44, AtMYB70, AtMYB73 and AtMYB77 share high structural similarity and participate in root system development [24,61,62]. Interestingly, we detected enhanced expression of AtMYB70, AtMYB73, and AtMYB77 in atmyb44 plants, compared with WT (Figure 3). It was earlier proposed that AtMYB44 is a functional paralog of AtMYB73 and AtMYB77 for auxin-mediated lateral root growth and development [61]. Even though the functional redundancy of AtMYB70 with AtMYB44 in root growth has not yet been examined, it is implicit that AtMYB70, AtMYB73 and AtMYB77 are redundant with AtMYB44 to coordinate adaptive root development under Pi-stress conditions.
As a previous report shows [25], the atmyb44 root appears to have slightly enhanced root growth performance under both Pi-sufficient and Pi-stress conditions compared to WT (Figure 4A,B, Figures S3 and S4). One proposed AtMYB44 function is as a negative regulator in abscisic acid (ABA) responses, which are involved in root growth inhibition [25,63,64]. AtMYB44 interacts with PYRABACTIN RESISTANCE 1-LIKE 8 (PYL8), identified as an ABA receptor, to regulate early ABA signaling and promote lateral root growth [25,61]. ABA signaling can play a role in enhancing the promoter activity of various auxin-responsive genes [64]. Although limited information is available regarding the role of ABA in Pi-starvation responses [65], it is plausible that AtMYB44 might inhibit ABA responses and activate auxin signaling to enhance root development in response to the imposed Pi-stress. However, our AtMYB44 OX lines did not show a clearly opposite phenotype with the atmyb44 line under Pi-stress, even though, based on the previous report, the expression level of MYB44 was 23- and 12-fold higher in AtMYB44 OX-1 and 2 lines compared with WT [25,33] (Figure 4, Figures S3 and S4). This result could not be explained as a role of AtMYB44 in Pi-starvation signaling; however, as AtMYB44 has been proposed to be involved in multiple signaling pathways, ectopic expression of AtMYB44 might result in aberrant ABA and auxin signaling to establish unidentified molecular responses under these Pi-stress conditions.

3.2. AtMYB44 mRNA Acts as a Systemic Pi Signaling Factor to Negatively Regulate Root Pi Transport Systems

In this study, we provide insight into the function of AtMYB44 as a negative regulator in systemic responses to Pi-stress, which might be associated with the promoter regions of PHT1;2 and PHT1;4 (Table S2). Enhanced PHT1;2 and PHT1;4 expression and elevated soluble Pi concentration were detected in atmyb44 plants, compared to WT (Figure 4C,D and Figure 5). It is noticeable that the soluble Pi concentration was higher in shoots and lower in roots of the atmyb44 mutant under Pi-sufficient conditions, compared with WT (Figure 4C,D). This suggests that, in Arabidopsis, AtMYB44 plays a negative role in root-to-shoot Pi transport under Pi-sufficient conditions. Hence, Pi translocation through the xylem might be enhanced in atmyb44 plants. Future research is needed to provide relevant evidence to verify the detailed binding mechanisms between AtMYB44 and the promoter regions of PHT1;2 and PHT1;4 under both Pi-sufficient and Pi-starvation conditions.
Interestingly, under Pi-stress conditions, although a similar level of soluble Pi concentration was detected in the shoots of WT and atmyb44, its level was higher in atmyb44 roots, and this result seems to be correlated with increased root biomass (Figure 4 and Figure S3). Additionally, shoot biomass of atmyb44 was significantly elevated under Pi-sufficient, but not Pi-limiting conditions (Figure 4). It is possible that AtMYB44 functions in roots as a negative regulator of PHT1;2 and PHT1;4 (Figure 5); thus, enhanced levels of PHT1;2 and PHT1;4 would increase the efficiency of Pi uptake and plant growth performance in atmyb44 plants under Pi-stress conditions. Taken together, it appears that AtMYB44 might play a negative role in Pi transport from root to shoot under Pi-sufficient conditions, but during a Pi-stress treatment, it might act as a negative regulator on Pi uptake in Arabidopsis.
The split-root assays demonstrated that AtMYB44 expression is systemically regulated by Pi-stress (Figure 6B). Consistent with a previous study [12], systemic responses of PHT1;2 and PHT1;4 were observed, and interestingly, such long-distance regulation was partially disrupted in the atmyb44 mutant background (Figure 6C,D). The mobility of AtMYB44 mRNA appeared to reduce the level of PHT1;2 and PHT1;4 transcript abundance in roots (Figure 7). In this regard, various RNA species, including mRNAs, small interfering RNAs, and non-coding RNAs, etc., have been shown to be translocated through the phloem, and some mobile RNA molecules can act as signaling agents in plant development and physiology [14,35,40,55,56,66,67,68,69,70,71]. For example, GIBBERELLIC ACID-INSENSITIVE mRNA is transported from the source to sink tissues and contributes to regulating leaf development [72,73]. Additionally, potato tuberization is regulated with the transportation of SP6A mRNA from potato leaves to the underground stolon [74,75]. The shoot-derived INDOLEACETIC ACID18 (IAA18), IAA28 and TRANSLATIONALLY CONTROLLED TUMOUR PROTEIN (TCTP) traffic into the roots to regulate the lateral root development [76,77,78].
In our study, we propose that mobile AtMYB44 mRNA serves as a long-distance phloem-based signal in the Pi-stress response (Figure 7). Although AtMYB44 lacked modified base 5-methylcytosine (m5C), CU- or tRNA-like motifs, which have been characterized as contributing to phloem mRNA mobility [79,80,81], our heterografting assay established the mobility of AtMYB44 mRNA in Arabidopsis (Figure 7 and Figure S5). As AtMYB44 and CsMYB44 protein have not been detected in the phloem exudate [82,83], it is likely that AtMYB44 mRNA and not protein serves as the signaling agent in Pi homeostasis. Although mobile AtMYB44 mRNA is involved in regulating PHT1 expression, in roots, the regulatory mechanism underlying its phloem mobility, in Pi acquisition and utilization, remains to be elucidated. Based on previous studies [80,81], the shoot-derived AtMYB44 mRNA could be transported through the phloem and then translated in the targeted root tissues to regulate Pi transport.
Our study showed enhanced AtMYB44 expression under Pi-stress conditions, and a negative role for AtMYB44 in PHT1 expression in Arabidopsis roots (Figure 8). As an increase in both AtMYB44 and PHT1 expression was detected under Pi-stress, this raises the question as to why plants would enhance AtMYB44 expression to repress the Pi transport system under Pi-stress conditions, even though one would expect these plants to increase their Pi uptake capacity to adapt under limited Pi input. Mobile AtMYB44 mRNA might play a role in fine-tuning the regulation of Pi homeostasis in response to Pi-stress for control over the energy balance between adaptive plant development and Pi uptake (Figure 8). Our current findings provide insight into plant Pi-stress regulatory pathways and further studies will be required to reveal the molecular mechanism by which such mobile AtMYB44 mRNA effect the ability of the plant to acquire and utilize Pi during Pi-stress conditions. Such information would be of value in genetic engineering of crops for improved yield performance under reduced Pi fertilizer applications.

4. Materials and Methods

4.1. Plant Materials

Arabidopsis plants were grown in controlled environment chambers under long-day conditions (16 h light/8 h dark, 120–150 μmol m−2 s−1 of photosynthetically active radiation), at temperatures of 22 °C day/18 °C night [84,85]. The T-DNA knock-out line (SALK_039074 [atmyb44]) for AT5G67300 was obtained from the Arabidopsis Biological Resource Center (ABRC, Columbus, OH, USA). The genotypes were confirmed using PCR analysis with appropriate primer sets (Table S1).

4.2. Growth Conditions and Pi-Stress Treatments

Arabidopsis plant lines were grown on solid medium (pH 5.7), in sand, or in a hydroponic culture system, as described previously [35,84,86,87,88,89]. In brief, Arabidopsis seeds were sterilized, germinated on solid medium with 500 µM NH4H2PO4 and then, at 7 days after germination (DAG), they were transferred onto fresh medium or medium with (NH4)2SO4 that partially or completely replaced NH4H2PO4. For hydroponically grown Arabidopsis plants, the tip of a 10 µL pipette was cut and then filled with 0.7% (w/v) agar, upon which sterilized seeds were sown, prior to setting them up on a floating board system. Hydroponic solution was replaced every 5 days. The solution for Pi-sufficient and starvation treatment contained 200 µM and 5 µM of NH4H2PO4, respectively. For growing Arabidopsis plants in sand, seeds were germinated on solid medium with 500 µM (Pi-sufficient) or 10 µM (Pi-starvation) of NH4H2PO4 for 14 days, followed by transplanting to silica sand. Arabidopsis plants were further grown in silica sand for 14 days with nutrient solution, which contained 500 µM (Pi-sufficient) or 10 µM (Pi-starvation) of NH4H2PO4, supplied to the roots. Images of root system architecture were captured with a Nikon D7200 (Nikon, Tokyo, Japan) digital camera. Acquired images were processed and analyzed using ImageJ software (version 1.53), as described previously [89].
Shoot and root tissues were collected from hydroponically cultured Arabidopsis plants and were used to measure biomass and Pi concentration, as described previously [86,87]. Collected shoot and root tissues were frozen in liquid nitrogen after measurement of fresh weight and then homogenized using a bead beater. Ground samples were digested with 5 M H2SO4, and then Pi concentrations were determined using a continuous flow analyzer (Skalar, Breda, The Netherlands), following the manufacturer’s instructions.
Four-week-old Arabidopsis plants were used for the split-root assays, as described previously [12,90], with modifications. Arabidopsis roots were divided into two parts and then immersed in two separate compartments, which contained either the same nutrient solution with 200 µM Pi (CP200) or 0 µM Pi (CP0), or a different nutrient solution with 200 µM Pi (SP200) and 0 µM Pi (SP0), for 7 days [12,90].

4.3. Phylogenetic Analysis

The amino acid sequences of AtMYBs were obtained from the Arabidopsis Information Resource Database (https://www.arabidopsis.org/, 4 November 2019) and aligned using MEGA 11 software. The phylogenetic tree was constructed using a neighbor-joining (NJ) method with 1000 bootstrap replicates.

4.4. β-Glucuronidase (GUS) Histochemical Analysis and Confocal Microscopy

The 2916 bp upstream region, which was from the ATG start codon of AtMYB44, was amplified from genomic DNA of Arabidopsis WT (Col-0), using the primer set listed in Table S1. The fragment was then inserted into the TOPO-D vector (Thermo Fisher Scientific, Waltham, MA, USA), followed by an LR clonase reaction (Invitrogen), to subclone the AtMYB44 promoter into pBGWFS7. The construct was introduced into Agrobacterium tumefaciens strain GV3101 to generate transgenic Arabidopsis plants. The GUS staining of transgenic plants, carrying a GUS reporter gene under the control of the AtMYB44 native promoter, was conducted, as described previously [84]. In brief, 12-day-old transgenic plants were immersed in 50 mM of sodium phosphate buffer (pH 7.0) with 1 mM K3Fe(CN)6, 1 mM K4Fe(CN)6, and 2 mM 5-bromo-4-chloro-3-indolyl β-D-glucuronide sodium salt and 10 mM EDTA (pH 8.0) and incubated at 37 °C. The chlorophyll was eliminated using 70% ethanol. T3 plants collected from three independent transgenic lines were used for GUS assays and imaged, using a THUNDER stereomicroscope (Leica, Wetzlar, Germany) and Zeiss Axioskop 2 Plus microscope.
For the confocal microscopy, propidium iodide (PI) (10 mg/mL) was used to stain the roots of an Arabidopsis seedling. GFP and PI were excited with 488 nm light, and emission was detected at 505–545 nm for GFP and 605–635 nm for PI. At least 6 Arabidopsis seedlings were examined for the confocal microscopy, and the same scanning conditions were used to take all images using Leica Stellaris 5.

4.5. Micrografting

Arabidopsis micrografting was performed, as described previously [76,91]. Briefly, hypocotyls of 5-day-old Arabidopsis seedlings, grown on 1/2 × MS medium with 0.8% agar, were cut on nylon membranes using a surgical blade. The scion and stock were placed together to connect the shoot and root. Grafted Arabidopsis plants were grown on 1/2 × MS medium with 1.5% agar for 5 days. Successfully grafted plants were transferred to 1/2 × MS medium with 0.8% agar for further studies.

4.6. RNA Extraction and qRT-PCR

Total RNA was extracted from Arabidopsis leaves and roots, using the TRIzol® Reagent (Thermo Fisher Scientific, Waltham, MA, USA), following the manufacturer’s instructions. Total RNA of 1 µg was used for cDNA synthesis with the SuperScript IV first-strand synthesis system (Invitrogen). The qRT-PCR analysis was conducted, as described previously [92]. Briefly, the qRT-PCR was performed with PowerUp™ SYBR™ Green Master Mix (Thermo Fisher Scientific, Waltham, MA, USA), using the QuantStudio™ 6 Flex Real-Time PCR Systems (Life Technologies), to detect AtMYB44, AtMYB70, AtMYB73, AtMYB77, PHT1;2, PHT1;4, and MGD3 with the primer sets listed in Table S1. AtActin was used as a reference gene for normalization of transcript levels. Transcript levels and ratios were calculated using the 2−∆Ct or the 2−∆∆Ct method, respectively. Statistical analyses were performed with the Student’s t-test and Tukey’s HSD (honestly significant difference) test. At least three biological and three technical replicates were used for qRT-PCR analyses.

Supplementary Materials

The following supporting information can be downloaded at: https://www.mdpi.com/article/10.3390/plants12203617/s1, Figure S1: Phylogenetic analysis of the A. thaliana MYB family; Figure S2: The AtMYB44 expression was increased in response to Pi-starvation stress; Figure S3: AtMYB44 is involved in primary and lateral root development; Figure S4: AtMYB44 serves as a potential negative regulator in shoot and root development; Figure S5: Mobility of AtMYB44 mRNA; Table S1: List of PCR primers used in this study; Table S2: Potential AtMYB44-mediated gene regulation in Arabidopsis.

Author Contributions

T.O., J.C. and B.-K.H. conceived the project; T.O., J.C. and B.-K.H. designed the experiments; T.O., J.C., Y.Z. and C.Q. conducted the experiments; B.-K.H. and L.V.K. provided technical advice. All authors contributed to perform the data analysis and interpretation; J.C. and T.O. prepared the draft and B.-K.H. revised the manuscript. All authors have read and agreed to the published version of the manuscript.

Funding

Financial support for this article was provided by the Canada Excellence Research Chair for Food Systems and Security (to L.V.K.), the Global Institute for Food Security (to L.V.K and B.-K.H.), Canada Foundation for Innovation—John R. Evans Leaders Fund (CFI#38103 to B.-K.H.), Natural Sciences and Engineering Research Council of Canada (#RGPIN-2019-04421 to BKH) and the New Frontiers in Research Fund NFRFE-2020-01108 (to B.-K.H.).

Data Availability Statement

The data in this study are available within the article.

Acknowledgments

Transgenic lines, overexpressing AtMYB44 (42-6 and 31-3 were referred to as AtMYB44 OX-1 and OX-2 in this study, respectively), were kindly provided by Huang Daiqing at the National Research Council of Canada, Saskatoon.

Conflicts of Interest

The authors declare no conflict of interest.

References

  1. MacDonald, G.K.; Bennett, E.M.; Potter, P.A.; Ramankutty, N. Agronomic phosphorus imbalances across the world’s croplands. Proc. Natl. Acad. Sci. USA 2011, 108, 3086–3091. [Google Scholar] [CrossRef] [PubMed]
  2. Withers, P.J.; Sylvester-Bradley, R.; Jones, D.L.; Healey, J.R.; Talboys, P.J. Feed the crop not the soil: Rethinking phosphorus management in the food chain. Environ. Sci. Technol. 2014, 48, 6523–6530. [Google Scholar] [CrossRef] [PubMed]
  3. Veneklaas, E.J.; Lambers, H.; Bragg, J.; Finnegan, P.M.; Lovelock, C.E.; Plaxton, W.C.; Price, C.A.; Scheible, W.R.; Shane, M.W.; White, P.J.; et al. Opportunities for improving phosphorus-use efficiency in crop plants. New Phytol. 2012, 195, 306–320. [Google Scholar] [CrossRef] [PubMed]
  4. Lopez-Arredondo, D.L.; Leyva-Gonzalez, M.A.; Gonzalez-Morales, S.I.; Lopez-Bucio, J.; Herrera-Estrella, L. Phosphate nutrition: Improving low-phosphate tolerance in crops. Annu. Rev. Plant Biol. 2014, 65, 95–123. [Google Scholar] [CrossRef] [PubMed]
  5. Kochian, L.V.; Piñeros, M.A.; Liu, J.; Magalhaes, J.V. Plant Adaptation to Acid Soils: The Molecular Basis for Crop Aluminum Resistance. Annu. Rev. Plant Biol. 2015, 66, 571–598. [Google Scholar] [CrossRef]
  6. Ham, B.K.; Chen, J.Y.; Yan, Y.; Lucas, W.J. Insights into plant phosphate sensing and signaling. Curr. Opin. Biotechnol. 2018, 49, 1–9. [Google Scholar] [CrossRef]
  7. Lynch, J.P. Root phenotypes for improved nutrient capture: An underexploited opportunity for global agriculture. New Phytol. 2019, 223, 548–564. [Google Scholar] [CrossRef]
  8. Morcuende, R.; Bari, R.; Gibon, Y.; Zheng, W.; Pant, B.D.; Blasing, O.; Usadel, B.; Czechowski, T.; Udvardi, M.K.; Stitt, M.; et al. Genome-wide reprogramming of metabolism and regulatory networks of Arabidopsis in response to phosphorus. Plant Cell Environ. 2007, 30, 85–112. [Google Scholar] [CrossRef]
  9. Lei, M.G.; Zhu, C.M.; Liu, Y.D.; Karthikeyan, A.S.; Bressan, R.A.; Raghothama, K.G.; Liu, D. Ethylene signalling is involved in regulation of phosphate starvation-induced gene expression and production of acid phosphatases and anthocyanin in Arabidopsis. New Phytol. 2011, 189, 1084–1095. [Google Scholar] [CrossRef]
  10. Puga, M.I.; Rojas-Triana, M.; de Lorenzo, L.; Leyva, A.; Rubio, V.; Paz-Ares, J. Novel signals in the regulation of Pi starvation responses in plants: Facts and promises. Curr. Opin. Plant Biol. 2017, 39, 40–49. [Google Scholar] [CrossRef]
  11. Li, L.; Liu, K.H.; Sheen, J. Dynamic Nutrient Signaling Networks in Plants. Annu. Rev. Cell Dev. Biol. 2021, 37, 341–367. [Google Scholar] [CrossRef] [PubMed]
  12. Thibaud, M.C.; Arrighi, J.F.; Bayle, V.; Chiarenza, S.; Creff, A.; Bustos, R.; Paz-Ares, J.; Poirier, Y.; Nussaume, L. Dissection of local and systemic transcriptional responses to phosphate starvation in Arabidopsis. Plant J. 2010, 64, 775–789. [Google Scholar] [CrossRef] [PubMed]
  13. Chen, J.; Ham, B.K. Systemic Signaling: A Role in Propelling Crop Yield. Plants 2022, 11, 1400. [Google Scholar] [CrossRef]
  14. Aung, K.; Lin, S.I.; Wu, C.C.; Huang, Y.T.; Su, C.L.; Chiou, T.J. pho2, a phosphate overaccumulator, is caused by a nonsense mutation in a MicroRNA399 target gene. Plant Physiol. 2006, 141, 1000–1011. [Google Scholar] [CrossRef] [PubMed]
  15. Pant, B.D.; Buhtz, A.; Kehr, J.; Scheible, W.R. MicroRNA399 is a long-distance signal for the regulation of plant phosphate homeostasis. Plant J. 2008, 53, 731–738. [Google Scholar] [CrossRef]
  16. Mudge, S.R.; Rae, A.L.; Diatloff, E.; Smith, F.W. Expression analysis suggests novel roles for members of the Pht1 family of phosphate transporters in Arabidopsis. Plant J. 2002, 31, 341–353. [Google Scholar] [CrossRef]
  17. Lin, S.I.; Chiang, S.F.; Lin, W.Y.; Chen, J.W.; Tseng, C.Y.; Wu, P.C.; Chiou, T.J. Regulatory network of microRNA399 and PHO2 by systemic signaling. Plant Physiol. 2008, 147, 732–746. [Google Scholar] [CrossRef]
  18. Nagarajan, V.K.; Jain, A.; Poling, M.D.; Lewis, A.J.; Raghothama, K.G.; Smith, A.P. Arabidopsis Pht1;5 Mobilizes Phosphate between Source and Sink Organs and Influences the Interaction between Phosphate Homeostasis and Ethylene Signaling. Plant Physiol. 2011, 156, 1149–1163. [Google Scholar] [CrossRef]
  19. Huang, T.K.; Han, C.L.; Lin, S.I.; Chen, Y.J.; Tsai, Y.C.; Chen, Y.R.; Chen, J.W.; Lin, W.Y.; Chen, P.M.; Liu, T.Y.; et al. Identification of downstream components of ubiquitin-conjugating enzyme PHOSPHATE2 by quantitative membrane proteomics in Arabidopsis roots. Plant Cell 2013, 25, 4044–4060. [Google Scholar] [CrossRef]
  20. Park, B.S.; Seo, J.S.; Chua, N.H. NITROGEN LIMITATION ADAPTATION recruits PHOSPHATE2 to target the phosphate transporter PT2 for degradation during the regulation of Arabidopsis phosphate homeostasis. Plant Cell 2014, 26, 454–464. [Google Scholar] [CrossRef]
  21. Martin, C.; Paz-Ares, J. MYB transcription factors in plants. Trends Genet. 1997, 13, 67–73. [Google Scholar] [CrossRef] [PubMed]
  22. Stracke, R.; Werber, M.; Weisshaar, B. The R2R3-MYB gene family in Arabidopsis thaliana. Curr. Opin. Plant Biol. 2001, 4, 447–456. [Google Scholar] [CrossRef] [PubMed]
  23. Dubos, C.; Stracke, R.; Grotewold, E.; Weisshaar, B.; Martin, C.; Lepiniec, L. MYB transcription factors in Arabidopsis. Trends Plant Sci. 2010, 15, 573–581. [Google Scholar] [CrossRef] [PubMed]
  24. Jung, C.; Seo, J.S.; Han, S.W.; Koo, Y.J.; Kim, C.H.; Song, S.I.; Nahm, B.H.; Choi, Y.D.; Cheong, J.J. Overexpression of AtMYB44 enhances stomatal closure to confer abiotic stress tolerance in transgenic Arabidopsis. Plant Physiol. 2008, 146, 623–635. [Google Scholar] [CrossRef]
  25. Jaradat, M.R.; Feurtado, J.A.; Huang, D.; Lu, Y.; Cutler, A.J. Multiple roles of the transcription factor AtMYBR1/AtMYB44 in ABA signaling, stress responses, and leaf senescence. BMC Plant Biol. 2013, 13, 192. [Google Scholar] [CrossRef]
  26. Persak, H.; Pitzschke, A. Dominant repression by Arabidopsis transcription factor MYB44 causes oxidative damage and hypersensitivity to abiotic stress. Int. J. Mol. Sci. 2014, 15, 2517–2537. [Google Scholar] [CrossRef]
  27. Zhao, Q.; Li, M.; Jia, Z.; Liu, F.; Ma, H.; Huang, Y.; Song, S. AtMYB44 Positively Regulates the Enhanced Elongation of Primary Roots Induced by N-3-Oxo-Hexanoyl-Homoserine Lactone in Arabidopsis thaliana. Mol. Plant Microbe Interact. 2016, 29, 774–785. [Google Scholar] [CrossRef]
  28. Zhou, X.; Zha, M.; Huang, J.; Li, L.; Imran, M.; Zhang, C. StMYB44 negatively regulates phosphate transport by suppressing expression of PHOSPHATE1 in potato. J. Exp. Bot. 2017, 68, 1265–1281. [Google Scholar] [CrossRef]
  29. Rubio, V.; Linhares, F.; Solano, R.; Martin, A.C.; Iglesias, J.; Leyva, A.; Paz-Ares, J. A conserved MYB transcription factor involved in phosphate starvation signaling both in vascular plants and in unicellular algae. Genes Dev. 2001, 15, 2122–2133. [Google Scholar] [CrossRef]
  30. Nilsson, L.; Muller, R.; Nielsen, T.H. Increased expression of the MYB-related transcription factor, PHR1, leads to enhanced phosphate uptake in Arabidopsis thaliana. Plant Cell Environ. 2007, 30, 1499–1512. [Google Scholar] [CrossRef]
  31. Devaiah, B.N.; Madhuvanthi, R.; Karthikeyan, A.S.; Raghothama, K.G. Phosphate starvation responses and gibberellic acid biosynthesis are regulated by the MYB62 transcription factor in Arabidopsis. Mol. Plant 2009, 2, 43–58. [Google Scholar] [CrossRef]
  32. Dai, X.Y.; Wang, Y.Y.; Yang, A.; Zhang, W.H. OsMYB2P-1, an R2R3 MYB Transcription Factor, Is Involved in the Regulation of Phosphate-Starvation Responses and Root Architecture in Rice. Plant Physiol. 2012, 159, 169–183. [Google Scholar] [CrossRef]
  33. Ruan, W.; Guo, M.; Xu, L.; Wang, X.; Zhao, H.; Wang, J.; Yi, K. An SPX-RLI1 Module Regulates Leaf Inclination in Response to Phosphate Availability in Rice. Plant Cell 2018, 30, 853–870. [Google Scholar] [CrossRef]
  34. Guo, M.; Zhang, Y.; Jia, X.; Wang, X.; Zhang, Y.; Liu, J.; Yang, Q.; Ruan, W.; Yi, K. Alternative splicing of REGULATOR OF LEAF INCLINATION 1 modulates phosphate starvation signaling and growth in plants. Plant Cell 2022, 34, 3319–3338. [Google Scholar] [CrossRef]
  35. Zhang, Z.L.; Zheng, Y.; Ham, B.K.; Chen, J.Y.; Yoshida, A.; Kochian, L.V.; Fei, Z.J.; Lucas, W.J. Vascular-mediated signalling involved in early phosphate stress response in plants. Nat. Plants 2016, 2, 16033. [Google Scholar] [CrossRef]
  36. Cheng, C.; Li, Q.; Wang, X.; Li, Y.; Qian, C.; Li, J.; Lou, Q.; Jahn, M.; Chen, J. Identification and Expression Analysis of the CsMYB Gene Family in Root Knot Nematode-Resistant and Susceptible Cucumbers. Front. Genet. 2020, 11, 550677. [Google Scholar] [CrossRef]
  37. Müller, R.; Morant, M.; Jarmer, H.; Nilsson, L.; Nielsen, T.H. Genome-wide analysis of the Arabidopsis leaf transcriptome reveals interaction of phosphate and sugar metabolism. Plant Physiol. 2007, 143, 156–171. [Google Scholar] [CrossRef]
  38. Bustos, R.; Castrillo, G.; Linhares, F.; Puga, M.I.; Rubio, V.; Perez-Perez, J.; Solano, R.; Leyva, A.; Paz-Ares, J. A central regulatory system largely controls transcriptional activation and repression responses to phosphate starvation in Arabidopsis. PLoS Genet. 2010, 6, e1001102. [Google Scholar] [CrossRef]
  39. Sun, L.; Song, L.; Zhang, Y.; Zheng, Z.; Liu, D. Arabidopsis PHL2 and PHR1 Act Redundantly as the Key Components of the Central Regulatory System Controlling Transcriptional Responses to Phosphate Starvation. Plant Physiol. 2016, 170, 499–514. [Google Scholar] [CrossRef]
  40. Thieme, C.J.; Rojas-Triana, M.; Stecyk, E.; Schudoma, C.; Zhang, W.; Yang, L.; Minambres, M.; Walther, D.; Schulze, W.X.; Paz-Ares, J.; et al. Endogenous Arabidopsis messenger RNAs transported to distant tissues. Nat. Plants 2015, 1, 15025. [Google Scholar] [CrossRef]
  41. Huang, D.; Jaradat, M.R.; Wu, W.; Ambrose, S.J.; Ross, A.R.; Abrams, S.R.; Cutler, A.J. Structural analogs of ABA reveal novel features of ABA perception and signaling in Arabidopsis. Plant J. 2007, 50, 414–428. [Google Scholar] [CrossRef] [PubMed]
  42. Brooks, M.D.; Juang, C.L.; Katari, M.S.; Alvarez, J.M.; Pasquino, A.; Shih, H.J.; Huang, J.; Shanks, C.; Cirrone, J.; Coruzzi, G.M. ConnecTF: A platform to integrate transcription factor-gene interactions and validate regulatory networks. Plant Physiol. 2021, 185, 49–66. [Google Scholar] [CrossRef] [PubMed]
  43. Daram, P.; Brunner, S.; Persson, B.L.; Amrhein, N.; Bucher, M. Functional analysis and cell-specific expression of a phosphate transporter from tomato. Planta 1998, 206, 225–233. [Google Scholar] [CrossRef]
  44. Muchhal, U.S.; Pardo, J.M.; Raghothama, K.G. Phosphate transporters from the higher plant Arabidopsis thaliana. Proc. Natl. Acad. Sci. USA 1996, 93, 10519–10523. [Google Scholar] [CrossRef] [PubMed]
  45. Okumura, S.; Mitsukawa, N.; Shirano, Y.; Shibata, D. Phosphate transporter gene family of Arabidopsis thaliana. DNA Res. 1998, 5, 261–269. [Google Scholar] [CrossRef] [PubMed]
  46. Raghothama, K.G. Phosphate transport and signaling. Curr. Opin. Plant Biol. 2000, 3, 182–187. [Google Scholar] [CrossRef] [PubMed]
  47. Nussaume, L.; Kanno, S.; Javot, H.; Marin, E.; Pochon, N.; Ayadi, A.; Nakanishi, T.M.; Thibaud, M.C. Phosphate Import in Plants: Focus on the PHT1 Transporters. Front. Plant Sci. 2011, 2, 83. [Google Scholar] [CrossRef] [PubMed]
  48. Plaxton, W.C.; Tran, H.T. Metabolic adaptations of phosphate-starved plants. Plant Physiol. 2011, 156, 1006–1015. [Google Scholar] [CrossRef]
  49. Bayle, V.; Arrighi, J.F.; Creff, A.; Nespoulous, C.; Vialaret, J.; Rossignol, M.; Gonzalez, E.; Paz-Ares, J.; Nussaume, L. Arabidopsis thaliana high-affinity phosphate transporters exhibit multiple levels of posttranslational regulation. Plant Cell 2011, 23, 1523–1535. [Google Scholar] [CrossRef]
  50. Chen, J.; Wang, Y.; Wang, F.; Yang, J.; Gao, M.; Li, C.; Liu, Y.; Liu, Y.; Yamaji, N.; Ma, J.F.; et al. The rice CK2 kinase regulates trafficking of phosphate transporters in response to phosphate levels. Plant Cell 2015, 27, 711–723. [Google Scholar] [CrossRef]
  51. Kobayashi, K.; Masuda, T.; Takamiya, K.; Ohta, H. Membrane lipid alteration during phosphate starvation is regulated by phosphate signaling and auxin/cytokinin cross-talk. Plant J. 2006, 47, 238–248. [Google Scholar] [CrossRef] [PubMed]
  52. Hamburger, D.; Rezzonico, E.; Petetot, J.M.C.; Somerville, C.; Poirier, Y. Identification and characterization of the Arabidopsis PHO1 gene involved in phosphate loading to the xylem. Plant Cell 2002, 14, 889–902. [Google Scholar] [CrossRef] [PubMed]
  53. Rouached, H.; Arpat, A.B.; Poirier, Y. Regulation of phosphate starvation responses in plants: Signaling players and cross-talks. Mol. Plant 2010, 3, 288–299. [Google Scholar] [CrossRef] [PubMed]
  54. Liu, T.Y.; Chang, C.Y.; Chiou, T.J. The long-distance signaling of mineral macronutrients. Curr. Opin. Plant Biol. 2009, 12, 312–319. [Google Scholar] [CrossRef]
  55. Ham, B.K.; Lucas, W.J. Phloem-Mobile RNAs as Systemic Signaling Agents. Annu. Rev. Plant Biol. 2017, 68, 173–195. [Google Scholar] [CrossRef]
  56. Zhang, Z.L.; Zheng, Y.; Ham, B.K.; Zhang, S.P.; Fei, Z.J.; Lucas, W.J. Plant lncRNAs are enriched in and move systemically through the phloem in response to phosphate deficiency. J. Integr. Plant Biol. 2019, 61, 492–508. [Google Scholar] [CrossRef]
  57. Yan, Y.; Ham, B.K. The Mobile Small RNAs: Important Messengers for Long-Distance Communication in Plants. Front. Plant Sci. 2022, 13, 928729. [Google Scholar] [CrossRef]
  58. Perez-Torres, C.A.; Lopez-Bucio, J.; Cruz-Ramirez, A.; Ibarra-Laclette, E.; Dharmasiri, S.; Estelle, M.; Herrera-Estrella, L. Phosphate availability alters lateral root development in Arabidopsis by modulating auxin sensitivity via a mechanism involving the TIR1 auxin receptor. Plant Cell 2008, 20, 3258–3272. [Google Scholar] [CrossRef]
  59. Huang, K.L.; Ma, G.J.; Zhang, M.L.; Xiong, H.; Wu, H.; Zhao, C.Z.; Liu, C.S.; Jia, H.X.; Chen, L.; Kjorven, J.O.; et al. The ARF7 and ARF19 Transcription Factors Positively Regulate PHOSPHATE STARVATION RESPONSE1 in Arabidopsis Roots. Plant Physiol. 2018, 178, 413–427. [Google Scholar] [CrossRef]
  60. Kranz, H.D.; Denekamp, M.; Greco, R.; Jin, H.; Leyva, A.; Meissner, R.C.; Petroni, K.; Urzainqui, A.; Bevan, M.; Martin, C.; et al. Towards functional characterisation of the members of the R2R3-MYB gene family from Arabidopsis thaliana. Plant J. 1998, 16, 263–276. [Google Scholar] [CrossRef]
  61. Zhao, Y.; Xing, L.; Wang, X.; Hou, Y.J.; Gao, J.; Wang, P.; Duan, C.G.; Zhu, X.; Zhu, J.K. The ABA receptor PYL8 promotes lateral root growth by enhancing MYB77-dependent transcription of auxin-responsive genes. Sci. Signal. 2014, 7, ra53. [Google Scholar] [CrossRef] [PubMed]
  62. Wan, J.; Wang, R.; Zhang, P.; Sun, L.; Ju, Q.; Huang, H.; Lu, S.; Tran, L.S.; Xu, J. MYB70 modulates seed germination and root system development in Arabidopsis. iScience 2021, 24, 103228. [Google Scholar] [CrossRef] [PubMed]
  63. Petricka, J.J.; Winter, C.M.; Benfey, P.N. Control of Arabidopsis root development. Annu. Rev. Plant Biol. 2012, 63, 563–590. [Google Scholar] [CrossRef]
  64. Belin, C.; Megies, C.; Hauserova, E.; Lopez-Molina, L. Abscisic Acid Represses Growth of the Arabidopsis Embryonic Axis after Germination by Enhancing Auxin Signaling. Plant Cell 2009, 21, 2253–2268. [Google Scholar] [CrossRef] [PubMed]
  65. Zhang, Y.; Li, T.T.; Wang, L.F.; Guo, J.X.; Lu, K.K.; Song, R.F.; Zuo, J.X.; Chen, H.H.; Liu, W.C. Abscisic acid facilitates phosphate acquisition through the transcription factor ABA INSENSITIVE5 in Arabidopsis. Plant J. 2022, 111, 269–281. [Google Scholar] [CrossRef]
  66. Hsieh, L.C.; Lin, S.I.; Shih, A.C.; Chen, J.W.; Lin, W.Y.; Tseng, C.Y.; Li, W.H.; Chiou, T.J. Uncovering small RNA-mediated responses to phosphate deficiency in Arabidopsis by deep sequencing. Plant Physiol. 2009, 151, 2120–2132. [Google Scholar] [CrossRef]
  67. Buhtz, A.; Pieritz, J.; Springer, F.; Kehr, J. Phloem small RNAs, nutrient stress responses, and systemic mobility. BMC Plant Biol. 2010, 10, 64. [Google Scholar] [CrossRef]
  68. Hao, L.; Zhang, Y.; Wang, S.; Zhang, W.; Wang, S.; Xu, C.; Yu, Y.; Li, T.; Jiang, F.; Li, W. A constitutive and drought-responsive mRNA undergoes long-distance transport in pear (Pyrus betulaefolia) phloem. Plant Sci. 2020, 293, 110419. [Google Scholar] [CrossRef]
  69. Xia, C.; Huang, J.; Lan, H.; Zhang, C. Long-Distance Movement of Mineral Deficiency-Responsive mRNAs in Nicotiana Benthamiana/Tomato Heterografts. Plants 2020, 9, 876. [Google Scholar] [CrossRef]
  70. Kitagawa, M.; Wu, P.; Balkunde, R.; Cunniff, P.; Jackson, D. An RNA exosome subunit mediates cell-to-cell trafficking of a homeobox mRNA via plasmodesmata. Science 2022, 375, 177–182. [Google Scholar] [CrossRef]
  71. Kehr, J.; Morris, R.J.; Kragler, F. Long-Distance Transported RNAs: From Identity to Function. Annu. Rev. Plant Biol. 2022, 73, 457–474. [Google Scholar] [CrossRef] [PubMed]
  72. Haywood, V.; Yu, T.S.; Huang, N.C.; Lucas, W.J. Phloem long-distance trafficking of GIBBERELLIC ACID-INSENSITIVE RNA regulates leaf development. Plant J. 2005, 42, 49–68. [Google Scholar] [CrossRef] [PubMed]
  73. Huang, N.C.; Yu, T.S. The sequences of Arabidopsis GA-INSENSITIVE RNA constitute the motifs that are necessary and sufficient for RNA long-distance trafficking. Plant J. 2009, 59, 921–929. [Google Scholar] [CrossRef] [PubMed]
  74. Banerjee, A.K.; Chatterjee, M.; Yu, Y.; Suh, S.G.; Miller, W.A.; Hannapel, D.J. Dynamics of a mobile RNA of potato involved in a long-distance signaling pathway. Plant Cell 2006, 18, 3443–3457. [Google Scholar] [CrossRef] [PubMed]
  75. Hannapel, D.J.; Banerjee, A.K. Multiple Mobile mRNA Signals Regulate Tuber Development in Potato. Plants 2017, 6, 8. [Google Scholar] [CrossRef]
  76. Notaguchi, M.; Wolf, S.; Lucas, W.J. Phloem-mobile Aux/IAA transcripts target to the root tip and modify root architecture. J. Integr. Plant Biol. 2012, 54, 760–772. [Google Scholar] [CrossRef]
  77. Toscano-Morales, R.; Xoconostle-Cazares, B.; Martinez-Navarro, A.C.; Ruiz-Medrano, R. Long distance movement of an Arabidopsis Translationally Controlled Tumor Protein (AtTCTP2) mRNA and protein in tobacco. Front. Plant Sci. 2014, 5, 705. [Google Scholar] [CrossRef]
  78. Branco, R.; Masle, J. Systemic signalling through translationally controlled tumour protein controls lateral root formation in Arabidopsis. J. Exp. Bot. 2019, 70, 3927–3940. [Google Scholar] [CrossRef]
  79. Ham, B.K.; Brandom, J.L.; Xoconostle-Cazares, B.; Ringgold, V.; Lough, T.J.; Lucas, W.J. A polypyrimidine tract binding protein, pumpkin RBP50, forms the basis of a phloem-mobile ribonucleoprotein complex. Plant Cell 2009, 21, 197–215. [Google Scholar] [CrossRef]
  80. Zhang, W.N.; Thieme, C.J.; Kollwig, G.; Apelt, F.; Yang, L.; Winter, N.; Andresen, N.; Walther, D.; Kragler, F. tRNA-Related Sequences Trigger Systemic mRNA Transport in Plants. Plant Cell 2016, 28, 1237–1249. [Google Scholar] [CrossRef]
  81. Yang, L.; Perrera, V.; Saplaoura, E.; Apelt, F.; Bahin, M.; Kramdi, A.; Olas, J.; Mueller-Roeber, B.; Sokolowska, E.; Zhang, W.; et al. m5C Methylation Guides Systemic Transport of Messenger RNA over Graft Junctions in Plants. Curr. Biol. 2019, 29, 2465–2476.e5. [Google Scholar] [CrossRef] [PubMed]
  82. Guelette, B.S.; Benning, U.F.; Hoffmann-Benning, S. Identification of lipids and lipid-binding proteins in phloem exudates from Arabidopsis thaliana. J. Exp. Bot. 2012, 63, 3603–3616. [Google Scholar] [CrossRef] [PubMed]
  83. Hu, C.Y.; Ham, B.K.; El-Shabrawi, H.M.; Alexander, D.; Zhang, D.B.; Ryals, J.; Lucas, W.J. Proteomics and metabolomics analyses reveal the cucurbit sieve tube system as a complex metabolic space. Plant J. 2016, 87, 442–454. [Google Scholar] [CrossRef] [PubMed]
  84. Ham, B.K.; Li, G.; Kang, B.H.; Zeng, F.; Lucas, W.J. Overexpression of Arabidopsis plasmodesmata germin-like proteins disrupts root growth and development. Plant Cell 2012, 24, 3630–3648. [Google Scholar] [CrossRef] [PubMed]
  85. Yan, Y.; Ham, B.K.; Chong, Y.H.; Yeh, S.D.; Lucas, W.J. A Plant SMALL RNA-BINDING PROTEIN 1 Family Mediates Cell-to-Cell Trafficking of RNAi Signals. Mol. Plant 2020, 13, 321–335. [Google Scholar] [CrossRef] [PubMed]
  86. Duan, K.; Yi, K.; Dang, L.; Huang, H.; Wu, W.; Wu, P. Characterization of a sub-family of Arabidopsis genes with the SPX domain reveals their diverse functions in plant tolerance to phosphorus starvation. Plant J. 2008, 54, 965–975. [Google Scholar] [CrossRef]
  87. Chen, J.; Liu, Y.; Ni, J.; Wang, Y.; Bai, Y.; Shi, J.; Gan, J.; Wu, Z.; Wu, P. OsPHF1 regulates the plasma membrane localization of low- and high-affinity inorganic phosphate transporters and determines inorganic phosphate uptake and translocation in rice. Plant Physiol. 2011, 157, 269–278. [Google Scholar] [CrossRef]
  88. Yan, J.; Chia, J.C.; Sheng, H.; Jung, H.I.; Zavodna, T.O.; Zhang, L.; Huang, R.; Jiao, C.; Craft, E.J.; Fei, Z.; et al. Arabidopsis Pollen Fertility Requires the Transcription Factors CITF1 and SPL7 That Regulate Copper Delivery to Anthers and Jasmonic Acid Synthesis. Plant Cell 2017, 29, 3012–3029. [Google Scholar] [CrossRef]
  89. Hoekenga, O.A.; Maron, L.G.; Pineros, M.A.; Cancado, G.M.; Shaff, J.; Kobayashi, Y.; Ryan, P.R.; Dong, B.; Delhaize, E.; Sasaki, T.; et al. AtALMT1, which encodes a malate transporter, is identified as one of several genes critical for aluminum tolerance in Arabidopsis. Proc. Natl. Acad. Sci. USA 2006, 103, 9738–9743. [Google Scholar] [CrossRef]
  90. Gansel, X.; Munos, S.; Tillard, P.; Gojon, A. Differential regulation of the NO3− and NH4+ transporter genes AtNrt2.1 and AtAmt1.1 in Arabidopsis: Relation with long-distance and local controls by N status of the plant. Plant J. 2001, 26, 143–155. [Google Scholar] [CrossRef]
  91. Melnyk, C.W. Grafting with Arabidopsis thaliana. Methods Mol. Biol. 2017, 1497, 9–18. [Google Scholar] [CrossRef]
  92. Ham, B.K.; Wang, X.; Toscano-Morales, R.; Lin, J.; Lucas, W.J. Plasmodesmal endoplasmic reticulum proteins regulate intercellular trafficking of Cucumber mosaic virus in Arabidopsis. J. Exp. Bot. 2023, 74, 4401–4414. [Google Scholar] [CrossRef]
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Figure 1. AtMYB44 is a potential functional homolog of CsMYB44. (A) The clade, which includes the closest MYB homologs of CsMYB44, in the phylogenic tree of the Arabidopsis MYB family, is shown in Figure S1. Numbers above the phylogenetic tree indicate posterior probabilities. (B) P1BSs, which are PHR1 binding motifs, predicted in the promoter regions of AtMYB44, AtMYB70 and AtMYB73, but not AtMYB77. Red bars indicate the P1BS motifs. (C,D) Relative expression of AtMYB44, AtMYB70, AtMYB73, and AtMYB77 in the shoot (C) and the root (D), under Pi-sufficient (500 µM) and Pi-starvation (10 µM) conditions. Arabidopsis seedlings were transplanted onto the medium with 500 µM, or 10 µM Pi, 5 days after germination on solid medium with 500 µM Pi. Shoot and root samples of Arabidopsis plants were harvested 7 days after Pi-sufficient (500 µM), or Pi-starvation (10 µM) treatment. Arabidopsis Actin was used as an internal control to normalize the qRT-PCR results. The data are presented as mean ± SD (three technical replicates and three technical repeats). Asterisks indicate significantly different values between Pi-sufficient and Pi-starvation conditions (Student’s t-test, p < 0.05).
Figure 1. AtMYB44 is a potential functional homolog of CsMYB44. (A) The clade, which includes the closest MYB homologs of CsMYB44, in the phylogenic tree of the Arabidopsis MYB family, is shown in Figure S1. Numbers above the phylogenetic tree indicate posterior probabilities. (B) P1BSs, which are PHR1 binding motifs, predicted in the promoter regions of AtMYB44, AtMYB70 and AtMYB73, but not AtMYB77. Red bars indicate the P1BS motifs. (C,D) Relative expression of AtMYB44, AtMYB70, AtMYB73, and AtMYB77 in the shoot (C) and the root (D), under Pi-sufficient (500 µM) and Pi-starvation (10 µM) conditions. Arabidopsis seedlings were transplanted onto the medium with 500 µM, or 10 µM Pi, 5 days after germination on solid medium with 500 µM Pi. Shoot and root samples of Arabidopsis plants were harvested 7 days after Pi-sufficient (500 µM), or Pi-starvation (10 µM) treatment. Arabidopsis Actin was used as an internal control to normalize the qRT-PCR results. The data are presented as mean ± SD (three technical replicates and three technical repeats). Asterisks indicate significantly different values between Pi-sufficient and Pi-starvation conditions (Student’s t-test, p < 0.05).
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Figure 2. AtMYB44 is expressed in response to Pi-starvation stress. Histochemical staining in 12-day-old transgenic Arabidopsis plants expressing the GFP-GUS reporter under the control of the AtMYB44 native promoter. Transgenic Arabidopsis seeds were germinated on solid medium with 500 µM Pi (Pi-sufficient medium) for 5 days and then transplanted to medium with 500 µM, or 10 µM Pi. Arabidopsis seedlings were collected 7 days after Pi-sufficient (500 µM), or Pi-starvation (10 µM) treatment. (A) GUS expression was barely detectable in Arabidopsis seedlings grown under Pi-sufficient (500 µM) conditions. (B) Under Pi-starvation (10 µM) conditions, GUS expression was observed in the primary root tip ((D), compared with (C) which showed GUS expression in the primary root tip under Pi-sufficient [500 µM] conditions), and Pi starvation also enhanced GUS expression in cotyledons (E), developing true leaves (F), lateral roots (G,H), and developing lateral root primordia (I,J). Dotted boxes indicate magnified regions for (C–J). Bars: 5 mm in (A,B), 500 µm in (E,F), and 50 µm in (C,D,G–J). In (K,L), AtMYB44 expression was increased in the epidermis, cortex layer and endodermis of the primary root tip under Pi-starvation (10 µM) conditions. In these representative confocal images, the GFP signal was enhanced in the primary root tip in response to the Pi starvation treatment (10 µM) (L) compared to growth on Pi-sufficient (500 µM) media (K) for 7 days. Arabidopsis seedling roots were stained with propidium iodide (PI, red). Epi, epidermis; cor, cortex layer; end, endodermis. Bar = 50 µm. (M,N): AtMYB44 expression was increased in both shoots (M) and roots (N) under Pi-starvation conditions. Arabidopsis seedlings (Col-0), germinated on agar medium with 500 µM Pi (Pi-sufficient medium) for 5 days, were transplanted to medium with 500 µM, or 10 µM Pi, and then collected over a 7-day time course of Pi-starvation treatment. The Arabidopsis Actin gene was used as an internal control to normalize the qRT-PCR results. The data are presented as mean ± SD (three biological replicates and three technical repeats).
Figure 2. AtMYB44 is expressed in response to Pi-starvation stress. Histochemical staining in 12-day-old transgenic Arabidopsis plants expressing the GFP-GUS reporter under the control of the AtMYB44 native promoter. Transgenic Arabidopsis seeds were germinated on solid medium with 500 µM Pi (Pi-sufficient medium) for 5 days and then transplanted to medium with 500 µM, or 10 µM Pi. Arabidopsis seedlings were collected 7 days after Pi-sufficient (500 µM), or Pi-starvation (10 µM) treatment. (A) GUS expression was barely detectable in Arabidopsis seedlings grown under Pi-sufficient (500 µM) conditions. (B) Under Pi-starvation (10 µM) conditions, GUS expression was observed in the primary root tip ((D), compared with (C) which showed GUS expression in the primary root tip under Pi-sufficient [500 µM] conditions), and Pi starvation also enhanced GUS expression in cotyledons (E), developing true leaves (F), lateral roots (G,H), and developing lateral root primordia (I,J). Dotted boxes indicate magnified regions for (C–J). Bars: 5 mm in (A,B), 500 µm in (E,F), and 50 µm in (C,D,G–J). In (K,L), AtMYB44 expression was increased in the epidermis, cortex layer and endodermis of the primary root tip under Pi-starvation (10 µM) conditions. In these representative confocal images, the GFP signal was enhanced in the primary root tip in response to the Pi starvation treatment (10 µM) (L) compared to growth on Pi-sufficient (500 µM) media (K) for 7 days. Arabidopsis seedling roots were stained with propidium iodide (PI, red). Epi, epidermis; cor, cortex layer; end, endodermis. Bar = 50 µm. (M,N): AtMYB44 expression was increased in both shoots (M) and roots (N) under Pi-starvation conditions. Arabidopsis seedlings (Col-0), germinated on agar medium with 500 µM Pi (Pi-sufficient medium) for 5 days, were transplanted to medium with 500 µM, or 10 µM Pi, and then collected over a 7-day time course of Pi-starvation treatment. The Arabidopsis Actin gene was used as an internal control to normalize the qRT-PCR results. The data are presented as mean ± SD (three biological replicates and three technical repeats).
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Figure 3. Transcript levels of AtMYB70, AtMYB73, and AtMYB77 are enhanced in atmyb44 knock-out mutants. Relative expression levels of AtMYB70 (A), AtMYB73 (B), and AtMYB77 (C) in WT (Col-0) and the atmyb44 mutant under Pi-sufficient (500 µM) and Pi-starvation (10 µM) conditions. Arabidopsis seedlings were transplanted onto medium with 500 µM, or 10 µM Pi 5 days after germination on solid medium with 500 µM Pi. Arabidopsis seedlings were harvested 7 days after Pi-sufficient (500 µM) or Pi-starvation (10 µM) treatment. Arabidopsis Actin was used as an internal control to normalize the qRT-PCR results. The data are presented as mean ± SD (three technical replicates and three technical repeats). The different lowercase letters indicate significant differences in relative gene expression levels, determined by the Tukey’s test (p < 0.05).
Figure 3. Transcript levels of AtMYB70, AtMYB73, and AtMYB77 are enhanced in atmyb44 knock-out mutants. Relative expression levels of AtMYB70 (A), AtMYB73 (B), and AtMYB77 (C) in WT (Col-0) and the atmyb44 mutant under Pi-sufficient (500 µM) and Pi-starvation (10 µM) conditions. Arabidopsis seedlings were transplanted onto medium with 500 µM, or 10 µM Pi 5 days after germination on solid medium with 500 µM Pi. Arabidopsis seedlings were harvested 7 days after Pi-sufficient (500 µM) or Pi-starvation (10 µM) treatment. Arabidopsis Actin was used as an internal control to normalize the qRT-PCR results. The data are presented as mean ± SD (three technical replicates and three technical repeats). The different lowercase letters indicate significant differences in relative gene expression levels, determined by the Tukey’s test (p < 0.05).
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Figure 4. AtMYB44 functions in plant growth under Pi-starvation conditions. (A) Shoot and (B) root biomass measurements on four-week-old Col-0, atmyb44, AtMYB44 OX-1 and OX2 lines, grown in a hydroponic culture system with high (200 µM) and low (5 µM) Pi concentrations. Shoot and root biomass was examined as fresh weight for each Arabidopsis plant. Soluble Pi concentration in (C) shoot and (D) root of four-week-old Col-0, atmyb44, AtMYB44 OX-1 and OX2 plants grown in a hydroponic culture system with high (200 µM) and low (5 µM) Pi concentrations. The data are presented as mean ± SD (three technical replicates and three technical repeats). The different lowercase letters indicate significant differences in biomass (A,B) and soluble Pi concentration (C,D), determined by the Tukey’s test (p < 0.05).
Figure 4. AtMYB44 functions in plant growth under Pi-starvation conditions. (A) Shoot and (B) root biomass measurements on four-week-old Col-0, atmyb44, AtMYB44 OX-1 and OX2 lines, grown in a hydroponic culture system with high (200 µM) and low (5 µM) Pi concentrations. Shoot and root biomass was examined as fresh weight for each Arabidopsis plant. Soluble Pi concentration in (C) shoot and (D) root of four-week-old Col-0, atmyb44, AtMYB44 OX-1 and OX2 plants grown in a hydroponic culture system with high (200 µM) and low (5 µM) Pi concentrations. The data are presented as mean ± SD (three technical replicates and three technical repeats). The different lowercase letters indicate significant differences in biomass (A,B) and soluble Pi concentration (C,D), determined by the Tukey’s test (p < 0.05).
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Figure 5. Expression of PHT1 is enhanced in atmyb44 roots. Relative expression level of PHT1;2 (A), PHT1;4 (B) and MGD3 (C) in WT (Col-0), atmyb44 and AtMYB44 OX-1 roots, under Pi-sufficient (500 µM) and Pi-starvation (10 µM) conditions. Arabidopsis seedlings were transplanted onto medium with 500 µM, or 10 µM Pi, 5 days after germination on solid medium with 500 µM Pi. Arabidopsis seedlings were harvested 7 days after Pi-sufficient (500 µM), or Pi-starvation (10 µM) treatment. Arabidopsis Actin was used as an internal control to normalize the qRT-PCR results. The data are presented as mean ± SD (three technical replicates and three technical repeats). The different lowercase letters indicate significant differences in relative gene expression levels, determined by Tukey’s test (p < 0.05).
Figure 5. Expression of PHT1 is enhanced in atmyb44 roots. Relative expression level of PHT1;2 (A), PHT1;4 (B) and MGD3 (C) in WT (Col-0), atmyb44 and AtMYB44 OX-1 roots, under Pi-sufficient (500 µM) and Pi-starvation (10 µM) conditions. Arabidopsis seedlings were transplanted onto medium with 500 µM, or 10 µM Pi, 5 days after germination on solid medium with 500 µM Pi. Arabidopsis seedlings were harvested 7 days after Pi-sufficient (500 µM), or Pi-starvation (10 µM) treatment. Arabidopsis Actin was used as an internal control to normalize the qRT-PCR results. The data are presented as mean ± SD (three technical replicates and three technical repeats). The different lowercase letters indicate significant differences in relative gene expression levels, determined by Tukey’s test (p < 0.05).
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Figure 6. AtMYB44 is a systemically regulated gene in response to an imposed Pi-starvation stress. Expression of endogenous AtMYB44 in roots of four-week-old WT (Col-0) and atmyb44 plants grown in split-root systems. (A) Schematic diagram illustrating the experimental design to detect systemic or local signaling under Pi-starvation conditions using a split-root system. CP200 and CP0 indicate homogenous Pi-sufficient (200 µM) and deficient (0 µM) treatment on roots, respectively. SP200 and SP0 indicate the half of the root system on a plant supplied with Pi-sufficient (200 µM) or deficient (0 µM) treatment, respectively. Arabidopsis roots were harvested 7 days after transferring plants into the split-root systems. (B) AtMYB44 expression is systemically regulated. AtMYB44 expression was examined in WT (Col-0) and atmyb44, using a split-root system. (C) PHT1;2 and (D) PHT1;4 expression in WT (Col-0) and atmyb44 using a split-root system. Arabidopsis Actin was used as an internal control to normalize the qRT-PCR results. The data are presented as mean ± SD (three technical replicates and three technical repeats). The different lowercase letters indicate significant differences in relative gene expression levels, determined by Tukey’s test (p < 0.05).
Figure 6. AtMYB44 is a systemically regulated gene in response to an imposed Pi-starvation stress. Expression of endogenous AtMYB44 in roots of four-week-old WT (Col-0) and atmyb44 plants grown in split-root systems. (A) Schematic diagram illustrating the experimental design to detect systemic or local signaling under Pi-starvation conditions using a split-root system. CP200 and CP0 indicate homogenous Pi-sufficient (200 µM) and deficient (0 µM) treatment on roots, respectively. SP200 and SP0 indicate the half of the root system on a plant supplied with Pi-sufficient (200 µM) or deficient (0 µM) treatment, respectively. Arabidopsis roots were harvested 7 days after transferring plants into the split-root systems. (B) AtMYB44 expression is systemically regulated. AtMYB44 expression was examined in WT (Col-0) and atmyb44, using a split-root system. (C) PHT1;2 and (D) PHT1;4 expression in WT (Col-0) and atmyb44 using a split-root system. Arabidopsis Actin was used as an internal control to normalize the qRT-PCR results. The data are presented as mean ± SD (three technical replicates and three technical repeats). The different lowercase letters indicate significant differences in relative gene expression levels, determined by Tukey’s test (p < 0.05).
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Figure 7. AtMYB44 plays a role in systemic PHT1;2 and PHT1;4 regulation. (A) Schematic diagram of Arabidopsis micrografting between atmyb44 and AtMYB44 OX-1 seedlings. (B) AtMYB44 is graft-transmissible from an AtMYB44 OX-1 scion to an atmyb44 rootstock. (C) Expression of AtPHT1;2 and AtPHT1;4 is decreased in the heterografted atmyb44 rootstock. Arabidopsis Actin was used as an internal control to normalize the qRT-PCR results. KO and OX-1 indicate atmyb44 mutant and AtMYB44 OX-1 line, respectively. The data are presented as mean ± SD (three technical replicates and three technical repeats). Asterisks indicate significantly different values with homografted atmyb44 plants. (Student’s t-test, p < 0.05).
Figure 7. AtMYB44 plays a role in systemic PHT1;2 and PHT1;4 regulation. (A) Schematic diagram of Arabidopsis micrografting between atmyb44 and AtMYB44 OX-1 seedlings. (B) AtMYB44 is graft-transmissible from an AtMYB44 OX-1 scion to an atmyb44 rootstock. (C) Expression of AtPHT1;2 and AtPHT1;4 is decreased in the heterografted atmyb44 rootstock. Arabidopsis Actin was used as an internal control to normalize the qRT-PCR results. KO and OX-1 indicate atmyb44 mutant and AtMYB44 OX-1 line, respectively. The data are presented as mean ± SD (three technical replicates and three technical repeats). Asterisks indicate significantly different values with homografted atmyb44 plants. (Student’s t-test, p < 0.05).
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Figure 8. Schematic model of mobile AtMYB44-mediated PHT1;2 and PHT1;4 regulation in Arabidopsis. (A) The mobile AtMYB44 transcript is long-distantly transported from source leaves to roots via the phloem and serves as a systemic signal to negatively regulate the expression of the Pi transporters, PHT1;2 and PHT1;4, in Arabidopsis roots. In the atmyb44 mutant, AtMYB44 mRNA is absent, thereby diminishing inhibition of PHT1;2 and PHT1;4 expression in roots. It results in increases of biomass and soluble Pi concentration in both shoots and roots of the atmyb44 mutant, compared to WT. (B) Under Pi-starvation conditions, PHR1 recognizes the promoter region of AtMYB44 and PHT1;2/PHT1;4 in shoots and roots, respectively, to induce those expressions. As AtMYB44 expression is abolished in the atmyb44 mutant, PHT1;2 and PHT1;4 expression is more enhanced in atmyb44 roots, compared to WT, due to absence of the negative regulatory factor, mobile AtMYB44 mRNA. Red darts and arrows indicate the increased level of designated gene expression and traits. Blue bars indicate a similar level of shoot biomass and shoot Pi concentration between WT and atmyb44 under Pi-starvation conditions. Question marks indicate the potential mechanisms that remain to be further investigated in the future. The Red X marks indicate systemic signaling mechanism, mediated by mobile AtMYB44 mRNA, are not functional in atmyb44 mutant.
Figure 8. Schematic model of mobile AtMYB44-mediated PHT1;2 and PHT1;4 regulation in Arabidopsis. (A) The mobile AtMYB44 transcript is long-distantly transported from source leaves to roots via the phloem and serves as a systemic signal to negatively regulate the expression of the Pi transporters, PHT1;2 and PHT1;4, in Arabidopsis roots. In the atmyb44 mutant, AtMYB44 mRNA is absent, thereby diminishing inhibition of PHT1;2 and PHT1;4 expression in roots. It results in increases of biomass and soluble Pi concentration in both shoots and roots of the atmyb44 mutant, compared to WT. (B) Under Pi-starvation conditions, PHR1 recognizes the promoter region of AtMYB44 and PHT1;2/PHT1;4 in shoots and roots, respectively, to induce those expressions. As AtMYB44 expression is abolished in the atmyb44 mutant, PHT1;2 and PHT1;4 expression is more enhanced in atmyb44 roots, compared to WT, due to absence of the negative regulatory factor, mobile AtMYB44 mRNA. Red darts and arrows indicate the increased level of designated gene expression and traits. Blue bars indicate a similar level of shoot biomass and shoot Pi concentration between WT and atmyb44 under Pi-starvation conditions. Question marks indicate the potential mechanisms that remain to be further investigated in the future. The Red X marks indicate systemic signaling mechanism, mediated by mobile AtMYB44 mRNA, are not functional in atmyb44 mutant.
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Olukayode, T.; Chen, J.; Zhao, Y.; Quan, C.; Kochian, L.V.; Ham, B.-K. Phloem-Mobile MYB44 Negatively Regulates Expression of PHOSPHATE TRANSPORTER 1 in Arabidopsis Roots. Plants 2023, 12, 3617. https://doi.org/10.3390/plants12203617

AMA Style

Olukayode T, Chen J, Zhao Y, Quan C, Kochian LV, Ham B-K. Phloem-Mobile MYB44 Negatively Regulates Expression of PHOSPHATE TRANSPORTER 1 in Arabidopsis Roots. Plants. 2023; 12(20):3617. https://doi.org/10.3390/plants12203617

Chicago/Turabian Style

Olukayode, Toluwase, Jieyu Chen, Yang Zhao, Chuanhezi Quan, Leon V. Kochian, and Byung-Kook Ham. 2023. "Phloem-Mobile MYB44 Negatively Regulates Expression of PHOSPHATE TRANSPORTER 1 in Arabidopsis Roots" Plants 12, no. 20: 3617. https://doi.org/10.3390/plants12203617

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