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Article

P2K1 Receptor, Heterotrimeric Gα Protein and CNGC2/4 Are Involved in Extracellular ATP-Promoted Ion Influx in the Pollen of Arabidopsis thaliana

by
Yansheng Wu
1,2,†,
Hongmin Yin
1,†,
Xinyue Liu
1,
Jiawei Xu
1,
Baozhi Qin
1,
Kaili Feng
1,
Erfang Kang
1,* and
Zhonglin Shang
1,*
1
Key Laboratory of Molecular & Cellular Biology of the Ministry of Education, College of Life Sciences, Hebei Normal University, Shijiazhuang 050024, China
2
College of Bioscience and Bioengineering, Xingtai University, Xingtai 054001, China
*
Authors to whom correspondence should be addressed.
†
These authors contributed equally to this work.
Plants 2021, 10(8), 1743; https://doi.org/10.3390/plants10081743
Submission received: 2 August 2021 / Revised: 20 August 2021 / Accepted: 20 August 2021 / Published: 23 August 2021
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Abstract

:
As an apoplastic signal, extracellular ATP (eATP) is involved in plant growth and development. eATP promotes tobacco pollen germination (PG) and pollen tube growth (PTG) by stimulating Ca2+ or K+ absorption. Nevertheless, the mechanisms underlying eATP-stimulated ion uptake and their role in PG and PTG are still unclear. Here, ATP addition was found to modulate PG and PTG in 34 plant species and showed a promoting effect in most of these species. Furthermore, by using Arabidopsis thaliana as a model, the role of several signaling components involved in eATP-promoted ion (Ca2+, K+) uptake, PG, and PTG were investigated. ATP stimulated while apyrase inhibited PG and PTG. Patch-clamping results showed that ATP promoted K+ and Ca2+ influx into pollen protoplasts. In loss-of-function mutants of P2K1 (dorn1-1 and dorn1-3), heterotrimeric G protein α subunit (gpa1-1, gpa1-2), or cyclic nucleotide gated ion channel (cngc2, cngc4), eATP-stimulated PG, PTG, and ion influx were all impaired. Our results suggest that these signaling components may be involved in eATP-promoted PG and PTG by regulating Ca2+ or K+ influx in Arabidopsis pollen grains.

1. Introduction

The apoplast, including the cell wall and intercellular space, plays essential roles in modulating plant cell growth and development due to the existence of numerous signaling molecules within the apoplastic matrix. In recent years, growing evidence has shown that adenosine triphosphate (ATP) is present in the apoplast and participates in physiological processes such as vegetative growth, development, and stress response [1,2,3,4]. eATP is involved in maintaining cell viability [5] and the growth rate of cultured cells [6], regulating the rate or direction of the growth of roots [7], hypocotyls [8,9], and cotton fibers [10]. It is also involved in modulating stomatal movement [11,12,13]. Some stresses induce eATP release as a “danger signal”, which in turn induces resistance responses to disease, hypotonic conditions, high salinity, and cold stress [14,15,16,17,18].
The signal transduction of eATP has been intensively investigated over the past two decades. Two lectin receptor kinases, P2K1 and P2K2, were identified to be eATP receptors in Arabidopsis thaliana [19,20] involved in eATP-induced immune responses [13,14,21]. Signal transducers in the plasma membrane (PM), including heterotrimeric G proteins [12,22], NADPH oxidase [23,24], and Ca2+ channels [6,23,25,26], were reported to be involved in eATP signal transduction. Several secondary messengers, e.g., ROS, H2O2, NO, and Ca2+ may be responsible for the eATP-induced intracellular responses that eventually alter plant growth and development [6,17,26,27,28,29].
PG and PTG are fundamental processes in plant sexual reproduction. Ion intake is the main factor affecting the two processes [30,31,32]. Through the regulation of turgor pressure, K+ ions play essential roles in PG and PTG. Proper K+ channel expression is essential for Arabidopsis pollen hydration on stigma [33]. K+ influx causes pollen tube apex bursting and the release of sperm cells to complete double fertilization [34] and endows pollen with competitive ability [35]. Excessively low or high K+ or Ca2+ concentration inhibited PG and PTG in vitro in Arabidopsis [36,37]. Inward K+ channels that drive K+ absorption by pollen cells are involved in PG and PTG [33,38,39,40]. Ca2+ is involved in modulating the activity of some inward K+ channels in pollen protoplasts [39,41].
As a component of the cell wall and a cytoplasmic messenger, Ca2+ ions play essential roles in PG and PTG [31,32,42,43,44,45]. Sufficient Ca2+ is necessary for PG and PTG. Pollen tubes emerge from the aperture where high cytosolic Ca2+ concentration ([Ca2+]cyt) is localized [42,46,47]. [Ca2+]cyt initiates pollen germination [46] and regulates the rate and direction of growth of pollen tubes [44,45,48,49,50,51]. Exocytosis occurs continuously during PG and PTG. Ca2+-regulated vesicle trafficking and fusion with the PM therefore play key roles in PG and PTG [51,52,53,54,55,56,57]. Ca2+ influx and signaling are responsible for stimuli-triggered or -regulated PG and PTG [58,59,60,61,62,63].
High concentrations of eATP show an inhibitory effect, while low concentrations of ATP show a promotive effect on PG and PTG [64,65,66]. We have reported that eATP stimulates the PG and PTG of Nicotiana tabacum by facilitating K+ or Ca2+ uptake [63]. Nevertheless, the universality of such an effect remains to be explored, and the signaling underlying eATP-stimulated PG and PTG remains unclear. Herein, we firstly investigated the response of pollen from 34 plant species to ATP addition and then elucidated the role of several signaling components in eATP-regulated PG and PTG of Arabidopsis thaliana.

2. Results

2.1. ATP Addition Impacts PG and PTG in Pollens from 34 Species

To verify the universality of eATP-regulated PG and PTG, we examined the effects of 0.1 mM ATP on PG and PTG of pollen grains from 34 species. Pollen germination rates increased significantly in 28 species (p < 0.05) and decreased significantly in 6 species (p < 0.05). Pollen tube length measurement results showed that tube growth was significantly promoted in 19 species (p < 0.05) and significantly inhibited in 5 species, while no effect was observed in 10 species (Figure 1).

2.2. eATP Regulates PG and PTG of Arabidopsis thaliana via K+ and Ca2+ Intake

To verify the role of ion uptake in eATP-promoted PG and PTG, Arabidopsis thaliana pollen was germinated in vitro, and the effects of apyrase or ATP addition on PG and PTG were investigated. In the basic medium, which contained 0.1 mM KCl, apyrase inhibited PG and PTG significantly. After 100 units/mL apyrase treatment, the pollen germination rate decreased from 39.2 ± 2.5% to 26.7 ± 3.4%, and the pollen tube length decreased from 16.9 ± 2.4 μm to 10.3 ± 1.8 μm (p < 0.05). Control treatment with heat-denatured apyrase or bovine serum albumin (BSA) did not affect PG or PTG (p > 0.05) (Figure 2A,D). At low K+ concentrations (0.02–0.1 mM), ATP supplementation (0.1 mM) promoted PG and PTG significantly, while at high K+ concentration (1.0 mM), ATP supplementation slightly inhibited PG but did not affect PTG (Figure 2B,E). To confirm that eATP supplementation promotes PG and PTG by increasing K+ uptake, 1 mM of the K+ channel blockers Ba2+, Cs+, or TEA (tetraethylammonium) was added into the basic medium containing 0.1 mM KCl. In these conditions, the effects of eATP on PG or PTG were significantly suppressed (p < 0.01) (Figure 2C,F).
To verify the role of Ca2+ in eATP-promoted PG and PTG, 0.1 mM ATP was added to medium containing EGTA, series of concentrations of Ca2+, or Ca2+ channel blockers. In 0.5 mM EGTA-containing medium, PG and PTG were significantly suppressed, and ATP supplementation did not have any effect. In medium containing 0.1 mM CaCl2, PG and PTG were both stimulated by 0.1 mM ATP. In medium containing 1 mM CaCl2, pollen tube growth was markedly stimulated, while pollen germination was suppressed by 0.1 mM ATP. In medium containing 0.1 mM Ca2+-permeable channel blockers (Gd3+ or La3+), resting PG and PTG were both suppressed, and added ATP did not have any effect on PG and PTG (Figure 3). These data indicate that eATP may promote PG and PTG by facilitating Ca2+ intake.
To verify the role of ATP hydrolytes in PG and PTG, 0.1 mM ADP, AMP, adenosine, adenine, or phosphate (Pi) was added to the medium containing 0.1 mM KCl or CaCl2. PG and PTG were not affected by these reagents in either KCl or CaCl2 medium (Figure S1A,C). To verify the effect of various ATP salts on PG and PTG, 0.1 mM ATP sodium, Tris, or magnesium salt was added to the medium containing 0.1 mM KCl or CaCl2. PG and PTG were significantly promoted by the three ATP salts (p < 0.05) in both the KCl and CaCl2 media (Figure S1B–D). To ensure that ATP acts as a signal rather than an energy carrier, 0.1 mM ATPγS, a weakly-hydrolyzable ATP analog, was added to the medium containing either 0.1 mM KCl or CaCl2. PG and PTG were significantly promoted by ATPγS (p < 0.05) in the KCl and CaCl2 media (Figure S1B–D).

2.3. ATP Stimulates K+ and Ca2+ Influx in Arabidopsis thaliana Pollen Protoplast

To confirm that eATP stimulates K+ uptake in pollen grains, whole-cell patch clamping was performed to detect the effect of eATP on K+ conductance in the PM. In pollen protoplasts, a time-dependent inward-rectifying K+ current was recorded at a negative voltage of more than −140 mV. The addition of 1 mM CsCl significantly suppressed the current intensity, confirming that the inward currents may be carried by K+ influx (Figure 4A). The addition of 0.1 mM ATP stimulated the inward K+ current: the maximum current intensity increased from −129 ± 32 pA to −254 ± 34 pA at −200 mV (n = 7, p < 0.05), and the open potential shifted to more positive (Figure 4B). In CsCl-pretreated protoplasts, the effect of ATP on the inward K+ currents was markedly suppressed. The maximum current intensity decreased from −270 ± 35 pA to −83 ± 18 pA at −200 mV (n = 7, p < 0.05) (Figure 4C).
To further confirm the promotion of eATP on the Ca2+ uptake of pollen grains, the effect of 0.1 mM ATP on inward Ca2+ conductance was investigated. The addition of 0.1 mM ATP strongly promoted Ca2+ influx in pollen protoplasts: the maximum inward current intensity at −200 mV increased from −147.6 ± 21.9 pA to −243.1 ± 22.8 pA (n = 7, p < 0.05) (Figure 5A,B). GdCl3 (1 mM) significantly suppressed Ca2+ conductance (Figure 5A,C, n = 7, p < 0.05). In Gd3+-pretreated pollen protoplasts, ATP did not stimulate Ca2+ inward conductance (Figure 5A,C, n = 7, p > 0.05).

2.4. P2K1 Receptor, Heterotrimeric G Protein α Subunit and Two CNGCs Are Involved in eATP-Regulated PG and PTG by Modulating K+ and Ca2+ Influx

To verify the role of P2K1 receptor in eATP-regulated PG and PTG, pollen grains of two P2K1 receptor (DORN1) null mutants, dorn1-1 and dorn1-3, were germinated in vitro. In 0.1 mM KCl-containing medium, 0.1 mM ATP addition did not affect the PG or PTG of dorn1-1 nor dorn1-3 mutants (Figure 6A,B). In 0.1 mM CaCl2-containing medium, ATP addition inhibited the PG of the two mutants but did not affect PTG in either (Figure 6E,F). In the pollen protoplasts of dorn1-1 and dorn1-3 mutants, K+ influx conductance was similar and exhibited weaker current intensity than wildtype pollen protoplasts. The addition of 0.1 mM ATP did not stimulate K+ conductance (Figure 6C,D). Ca2+ current intensity in pollen protoplasts of both mutants was weaker than that in wildtype, and the addition of 0.1 mM ATP did not stimulate Ca2+ conductance in either mutant (Figure 6G,H).
To verify the role of heterotrimeric G protein in eATP-regulated PG and PTG, pollen grains of two heterotrimeric Gα subunit null mutants, gpa1-1 and gpa1-2, were germinated in vitro. In 0.1 mM KCl or CaCl2 containing medium, the addition of 0.1 mM ATP did not promote PG or PTG in gpa1-1 and gpa1-2 mutants (Figure 7A–F). In pollen protoplasts of gpa1-1 and gpa1-2 mutants, K+ influx conductance was similar to that of wildtype pollen protoplasts. The addition of 0.1 mM ATP did not stimulate K+ conductance. Ca2+ current intensity in the pollen protoplasts of both mutants was weaker than that in wildtype, and the addition of 0.1 mM ATP did not stimulate Ca2+ conductance in either mutant (Figure 7C–H).
To verify the role of CNGC in eATP-regulated PG and PTG, pollen grains of two CNGC null mutants, cngc2 and cngc4, were germinated in vitro. In 0.1 mM KCl- or CaCl2-containing medium, the addition of 0.1 mM ATP did not stimulate PG or PTG in cngc2 or cngc4 mutants, while in 0.1 mM CaCl2-containing medium, PTG in cngc2 mutants was suppressed by ATP (Figure 8A–F). In the pollen protoplasts of cngc2 and cngc4 mutants, K+ influx conductance was weaker than in wildtype pollen protoplasts, and the addition of 0.1 mM ATP did not stimulate K+ conductance. Ca2+ current intensity in pollen protoplasts of both mutants was weaker than in wildtype, and the addition of 0.1 mM ATP did not stimulate Ca2+ conductance in either mutant (Figure 8C–H).

3. Discussion

3.1. eATP Regulates PG and PTG in Dozens of Plant Species

eATP plays a role in vegetative and reproductive tissue cells in plants. The addition of mM levels of ATP inhibited PG and PTG [64,65], while low concentrations of eATP stimulated PG and PTG [63,66]. Here, the responses of 34 plant species in terms of PG and PTG pointed to a dual effect of eATP: eATP had a positive effect on the pollen of most plant species, while had an inhibitory effect on the pollen of a few other species. Such a dual regulatory effect of eATP had been noticed in various plant systems [2,15,67]. The dual effect might result from the sensitivity of pollen to eATP. In most species, PG and PTG were promoted or inhibited simultaneously. Nevertheless, the responses of PG and PTG to ATP were not consistent. PG in Paeonia lactiflora, Magnolia denudata, Robinia pseudoacacia, Clivia miniata, and Pinus tabuliformis was promoted by eATP, but PTG did not change markedly. PG in Jasminum nudiflorum, Malus halliana, and Orychophragmus violaceus was promoted by ATP, whereas PTG was inhibited. For Kolkwitzia amabilis and Cotoneaster horizontalis, PG was inhibited by ATP, but PTG was not affected. These results revealed the universality of eATP’s regulatory effect on PG and PTG. Further research into the mechanism of eATP-regulated PG or PTG will shed light on the mechanisms that regulate plant sexual reproduction.

3.2. ATP Regulates PG and PTG of Arabidopsis thaliana

It had been reported that eATP regulates PG and PTG in Picea meyeri [66] and Nicotiana tabacum [63]. However, null mutants of eATP signaling components are difficult to generate in these species. Here, Arabidopsis pollen grains were used to verify the role of eATP in PG and PTG, and several mutants of eATP signaling components were used to clarify the role of these molecules in PG, PTG, and ion influx.
The addition of apyrase inhibited PG and PTG (Figure 2), indicating that endogenous eATP may be involved in maintaining PG and PTG. Endogenous eATP may be secreted during pollen development. The addition of ATP stimulated PG and PTG, indicating that endogenous eATP might be not sufficient and that PG and PTG can be promoted by increasing eATP level. Our finding that the addition of high levels of ATP inhibited the PG and PTG of Arabidopsis thaliana is in agreement with previous reports [64,65]. These reports used a high concentration of ATP (>1 mM), compared to the lower concentration of 0.1 mM ATP added here, which stimulated PG and PTG. These contrasting results indicate that, in a certain concentration range, eATP acts as a positive regulator. ATP hydrolytes, including ADP, AMP, and adenosine, did not affect PG or PTG, indicating that ATP hydrolysis is unnecessary for this regulatory effect. The addition of ADP stimulated some reactions that are evoked by eATP [3,23,25,68,69]. In our previous work, ADP was found to promote the PG and PTG of tobacco [63]. The results presented here indicate that Arabidopsis thaliana pollen may respond to ATP differently than tobacco pollen. A weakly hydrolyzable ATP analog, ATPγS, promoted PG and PTG of Arabidopsis thaliana similarly to ATP, confirming that ATP may function in its intact form as a signaling molecule. Various ATP salts showed similar positive effects on PG and PTG (Figure S1), indicating that the cations in these salts did not affect PG or PTG.

3.3. K+/Ca2+ Influx Mediates ATP Regulation of PG and PTG

In our previous work, we demonstrated the existence of eATP-regulated K+ and Ca2+ uptake in tobacco pollen [63]. Here, we found that K+ and Ca2+ uptake is necessary for resting or eATP-stimulated PG and PTG in Arabidopsis thaliana. Similar to the results in tobacco pollen, we found that ATP promoted PG and PTG in medium containing low concentrations of K+ or Ca2+ and inhibited PG and PTG in medium containing high concentrations of K+ or Ca2+. In medium containing 1 mM CaCl2, the pollen tube growth of tobacco was inhibited, while the pollen tube growth of Arabidopsis was strongly promoted (Figure 3B). In tobacco pollen, 0.1 mM Ca2+ channel blockers weakly suppressed eATP-promoted ion influx and PG and PTG, while in Arabidopsis thaliana, 0.1 mM Ca2+ channel blockers almost entirely blocked ATP-induced Ca2+ influx and PG and PTG. These results indicate that K+ and Ca2+ influx through ion channels may be a central event in PG and PTG, that endogenous eATP is necessary for maintaining resting ion uptake, that apyrase decreases eATP levels, and that decreased ion influx might explain apyrase-inhibited PG and PTG. The positive effects of ATP-supplementation on PG and PTG may partially result from increased ion absorption. The proper influx and accumulation of ions is essential for PG and PTG, while the overload of ions suppresses PG and PTG [32,33,37,40,45]. The data presented here suggest that, when eATP or ion concentrations are above normal levels, the overload of K+ or/and Ca2+ influx may inhibit PG and PTG.

3.4. Signaling Underlying ATP-Regulated PG and PTG of Arabidopsis thaliana

P2K1 receptor DORN1 was the first reported eATP receptor and is involved in plant immune and stress responses [13,14,21]. However, the role of the P2K1 receptor in sexual reproduction has not been investigated, although DORN1 is expressed in flowers (Figure S2). Results here showed that DORN1 is involved in PG and PTG. In 0.1 mM KCl-containing medium, the resting pollen germination rate and pollen tube length were similar between wildtype and both DORN1-null mutants, while in 0.1 mM CaCl2-containing medium, the pollen germination rate of both mutants was significantly lower than in wildtype, indicating that DORN1 is necessary for maintaining Ca2+ uptake and resting pollen germination, possibly through interactions with endogenous eATP. Patch clamping showed that resting K+ and Ca2+ current intensities were weaker than those in wildtype, demonstrating a role of DORN1 in maintaining the resting ion influx. Added ATP did not promote PG, PTG, or ion influx in dorn1-1 and dorn1-3, indicating that DORN1 plays a key role in ATP-regulated PG and PTG through regulating K+/Ca2+ influx in pollen cells. DORN1 is involved in eATP-regulated intracellular Ca2+ concentration elevation in Arabidopsis root cells [19,26,70,71]. The results here provided new evidence for a role for DORN1 in eATP-evoked Ca2+ signaling in reproductive cells as well. Heterotrimer G protein is involved in eATP-regulated root growth and stomatal movement and acts by regulating Ca2+ influx [3,12,22,72,73]. Heterotrimeric G protein-regulated PG, PTG, and Ca2+ influx in Arabidopsis thaliana was reported in our previous work [61]. Nevertheless, the upstream regulator that governs the heterotrimeric G protein is still unknown. The data presented here indicates that eATP may be an upstream regulator of heterotrimeric G protein in pollen cells, suggesting that eATP-stimulated G protein activation may play similar roles in vegetable and reproductive growth. The resting pollen germination rate and pollen tube length of gpa1-1 and gpa1-2 mutants were lower than those in wildtype, and the addition of ATP did not promote PG or PTG in either mutant, indicating that Gα may play a key role in eATP-regulated PG and PTG. In the protoplasts of both null mutants, resting K+ or Ca2+ current intensities were slightly weaker than those in wildtype, and the addition of ATP did not stimulate K+ or Ca2+ conductance, indicating that Gα may be involved in eATP-regulated ion influx. These data provide new evidence that heterotrimeric G protein is involved in eATP-regulated PG and PTG through regulating K+ or Ca2+ influx.
As channels permeable to divalent cations and K+, CNGCs had been reported to participate in key processes involved in plant growth, development, and stress responses, including apical growth, the vegetative development of plants, sexual reproduction, immunity, response to drought, and temperature stress [26,74,75,76,77]. CNGC2 and CNGC4 form ion channels by heterodimerization in Arabidopsis thaliana, after which they mediate ion influx and function in plant growth and pathogen defense [78,79,80]. In our preliminary experiments, the responses of pollen from several CNGC null mutants to ATP supplementation were investigated. Most mutants responded to eATP similarly to wildtype (data not shown). Only mutants for CNGC2 and CNGC4 responded to eATP different from Col-0 pollen. The resting pollen germination rates of cngc2 or cngc4 mutants were lower than that of wildtype, indicating that ion channels containing CNGC2 and CNGC4 are essential for maintaining Ca2+ and K+ uptake. In pollen grains from both mutants, the addition of ATP did not promote PG or PTG, indicating that CNGC2 and CNGC4 may play key roles in eATP-stimulated PG and PTG. Patch clamping data showed that resting K+ and Ca2+ conductance in mutants was weaker than in wildtype, confirming that resting ion influx may be mediated by ion channels containing CNGC2 and CNGC4. The addition of ATP did not stimulate K+ or Ca2+ conductance in the pollen protoplasts of cngc2 or cngc4 mutants, indicating that eATP-stimulated ion influx may be mediated by CNGC2/CNGC4-containing ion channels. Single null mutants of CNGC2 or CNGC4 showed impaired resting and eATP-stimulated ion influx, indicating that the heterodimerization of these two proteins is necessary for the construction of functional ion channels. It was reported that CNGC18 and CNGC16 are involved in the pollen development, germination and tube growth in Arabidopsis thaliana [59,81,82], whether these CNGCs are involved in eATP signaling need to be further investigated.
Our results confirmed which components are involved in eATP-stimulated PG, PTG, and ion flux and provided new clues to help elucidate the mechanisms of eATP-regulated reproduction. Based on these results, it is reasonable to speculate that eATP first binds the P2K1 receptor, then stimulates heterotrimer G protein, then activated Gα stimulates CNGC2/CNGC4, finally leading to increased Ca2+/K+ influx and the promotion of PG and PTG. How these components are connected remains unclear. Some receptor-like kinases directly bind and phosphorylate heterotrimeric G protein or activate heterotrimeric G protein through RGS1 (regulator of G protein signaling 1) [83,84,85]. Hence, the interaction of DORN1 and RGS1 (or heterotrimeric Gα) need to be carefully investigated before we can draw a conclusion. Heterotrimeric G protein is involved in the regulation of ion flux in plant cells [86]; however, whether heterotrimeric G protein directly activates ion channels or does so indirectly through altering membrane potential or generating cytoplasmic messengers (e.g., ROS or NO) needs to be clarified in the future.

4. Materials and Methods

4.1. Plant Materials

Pollen grains of 34 plant species (Table 1) were collected from newly opened flowers and then stored (adding silica gel as a dehydrator) at −20 °C.
Arabidopsis thaliana plants were grown in a greenhouse running at 22 °C with illumination intensity of 120–130 μmol·m−2·s−1, relative humidity of 70%, and a 16/8 h light/dark cycle.

4.2. In Vitro Pollen Germination

The basic medium contained 18% sucrose and had a pH of 7.0. Nutrient salts were added according to individual experimental aims. All reagents were dissolved in de-ionized water, and 0.5% agarose was added to solidify the medium for pollen germination.
Pollen grains were suspended in a basic medium and spread onto the surface of a solid medium. Then, pollen grains were incubated in the dark at 28 °C with a relative humidity of 100%. The incubation duration varied among different species since the time needed to reach maximum germination rate for each species is different (see detail in Table 1). After incubation, pollen grains were photographed with a DS-Fi1c imaging system equipped to a microscope (Nikon Eclipse 80i, Japan). Images were analyzed with NIS-Element BR 4.0 software to count germinated pollen grains and measure pollen tube length. In each experiment, no less than 300 pollen grains were counted to obtain germination rate (pollen grains with emerging tubes longer than 5 μm were considered as germinated pollen), and the lengths of no less than 150 pollen tubes were measured. Data from 3 replicates were calculated to obtain mean values. Data was analyzed with Statistica 8.0 software.

4.3. Protoplast Isolation

Pollen grains of Arabidopsis thaliana were incubated at 28 °C in a bath solution (20 mM CaCl2, 5 mM MES, 1.5 M sorbitol, pH 5.8), which contained 1.5% cellulase (Onozuka RS, Yakult, Japan) and 1% macerozyme (R-10, Yakult, Japan). After 1.5 h, the isolated pollen protoplasts were centrifuged and washed with the bath solution twice.

4.4. Patch-Clamp Recording

All patch-clamp solutions were adjusted to 1.5 Osm/kg with sorbitol. For K+ current detection, the bath solution specifications were 10 mM KC6H11O7, 5 mM Mes, and pH 5.8., and the pipette solution specifications were 100 mM KC6H11O7, 0.1 mM CaCl2, 2 mM MgCl2, 10 mM Hepes, 2 mM Mg·ATP, 1.1 mM EGTA, 4 mM KOH, and pH 7.2. For Ca2+ current detection, the bath solution specifications were 20 mM CaCl2, 5 mM Mes, and pH 5.8, and the pipette solution specifications were 0.5 mM CaCl2, 8.5 mM Ca(OH)2, 2 mM Mg∙ATP, 0.5 mM ATP∙Tris, 10 mM BAPTA, 15 mM Hepes, and pH 7.2.
Patch-clamp recording methods were manipulated according to Véry & Davies [87]. Glass pipettes (World Precision Instruments, FL, USA) were pulled with a vertical puller (PC-10, Narishige, Japan). A whole-cell voltage clamping configuration was used. Current signal was recorded with an AXON 200B amplifier (AXON Instruments, IL, USA) equipped with Digidata 1440A data acquisition system (AXON Instruments, IL, USA), which was controlled by Clampex 10.3 software (AXON Instruments, IL, USA). Data was sampled at 1 kHz and filtered at 200 Hz. Voltage-clamp protocols included a series of depolarizing and/or hyperpolarizing steps of 1.5 s from a holding potential in the range of 0 to −200 mV. Current–voltage relationships (I-V curves) were then constructed with total whole-cell currents measured after 1.5 s step-voltage clamping. Data were analyzed with Microcal Origin 6.0.

Supplementary Materials

The following are available online at https://www.mdpi.com/article/10.3390/plants10081743/s1, Figure S1: The effect of ATP, ATP agonist or hydrolytes on PG and PTG of Arabidopsis thaliana. Figure S2: The expression pattern of DORN 1 in Arabidopsis thaliana.

Author Contributions

Y.W., Z.S., and E.K. conceived of the original research project and selected methods. Z.S. supervized the experiments. Y.W., H.Y., and X.L. performed most of the experiments. J.X., B.Q., and K.F. provided technical assistance. All authors have read and agreed to the published version of the manuscript.

Funding

This research was funded by National Natural Science Foundation of China (Grant number 31871409, 31800233).

Institutional Review Board Statement

Not applicable.

Informed Consent Statement

Not applicable.

Data Availability Statement

The study did not report any data.

Acknowledgments

We sincerely thank Julia Davies in University of Cambridge, Alan Jones in University of North Carolina, and Bing Li in Hebei Normal University for offering the mutants used in our work.

Conflicts of Interest

The authors declare no conflict of interest.

References

  1. Cao, Y.; Tanaka, K.; Nguyen, C.T.; Stacey, G. Extracellular ATP is a central signaling molecule in plant stress responses. Curr. Opin. Plant Biol. 2014, 20, 82–87. [Google Scholar] [CrossRef] [PubMed]
  2. Tanaka, K.; Choi, J.; Cao, Y.; Stacey, G. Extracellular ATP acts as a damage-associated molecular pattern (DAMP) signal in plants. Front. Plant Sci. 2014, 5, 446. [Google Scholar] [CrossRef] [Green Version]
  3. Clark, G.; Roux, S.J. Role of Ca2+ in mediating plant responses to extracellular ATP and ADP. Int. J. Mol. Sci. 2018, 19, 3590. [Google Scholar] [CrossRef] [Green Version]
  4. Pietrowska-Borek, M.; Dobrogojski, J.; Sobieszczuk-Nowicka, E.; Borek, S. New insight into plant signaling: Extracellular ATP and uncommon nucleotides. Cells 2020, 9, 345. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  5. Chivasa, S.; Ndimba, B.K.; Simon, W.J.; Lindsey, K.; Slabas, A.R. Extracellular ATP functions as an endogenous external metabolite regulating plant cell viability. Plant Cell 2005, 17, 3019–3034. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  6. Wu, S.J.; Liu, Y.S.; Wu, J.Y. The signaling role of extracellular ATP and its dependence on Ca2+ flux in elicitation of Salvia miltiorrhiza hairy root cultures. Plant Cell Physiol. 2008, 49, 617–624. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  7. Kim, S.Y.; Sivaguru, M.; Stacey, G. Extracellular ATP in plants. Visualization, localization, and analysis of physiological significance in growth and signaling. Plant Physiol. 2006, 142, 984–992. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  8. Tonon, C.; Cecilia Terrile, M.; Jose Iglesias, M.; Lamattina, L.; Casalongue, C. Extracellular ATP, nitric oxide and superoxide act coordinately to regulate hypocotyl growth in etiolated Arabidopsis seedlings. J. Plant Physiol. 2010, 167, 540–546. [Google Scholar] [CrossRef]
  9. Zhu, R.; Dong, X.; Xue, Y.; Xu, J.; Zhang, A.; Feng, M.; Zhao, Q.; Xia, S.; Yin, Y.; He, S.; et al. Redox-Responsive Transcription Factor 1 (RRFT1) is involved in extracellular ATP-regulated Arabidopsis thaliana seedling growth. Plant Cell Physiol. 2020, 61, 685–698. [Google Scholar] [CrossRef] [PubMed]
  10. Clark, G.; Torres, J.; Finlayson, S.; Guan, X.; Handley, C.; Lee, J.; Kays, J.E.; Chen, Z.J.; Roux, S.J. Apyrase (nucleoside triphosphate-diphosphohydrolase) and extracellular nucleotides regulate cotton fiber elongation in cultured ovules. Plant Physiol. 2010, 152, 1073–1083. [Google Scholar] [CrossRef] [Green Version]
  11. Clark, G.; Fraley, D.; Steinebrunner, I.; Cervantes, A.; Onyirimba, J.; Liu, A.; Torres, J.; Tang, W.; Kim, J.; Roux, S.J. Extracellular nucleotides and apyrases regulate stomatal aperture in Arabidopsis. Plant Physiol. 2011, 156, 1740–1753. [Google Scholar] [CrossRef] [Green Version]
  12. Hao, L.H.; Wang, W.X.; Chen, C.; Wang, Y.F.; Liu, T.; Li, X.; Shang, Z.L. Extracellular ATP promotes stomatal opening of Arabidopsis thaliana through heterotrimeric G protein α subunit and reactive oxygen species. Mol. Plant 2012, 5, 852–864. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  13. Chen, D.; Cao, Y.; Li, H.; Kim, D.; Ahsan, N.; Thelen, J.; Stacey, G. Extracellular ATP elicits DORN1-mediated RBOHD phosphorylation to regulate stomatal aperture. Nat. Commun. 2017, 8, 2265. [Google Scholar] [CrossRef] [Green Version]
  14. Choi, J.; Tanaka, K.; Liang, Y.; Cao, Y.; Lee, S.Y.; Stacey, G. Extracellular ATP, a danger signal, is recognized by DORN1 in Arabidopsis. Biochem. J. 2014, 463, 429–437. [Google Scholar] [CrossRef]
  15. Chivasa, S.; Murphy, A.M.; Hamilton, J.M.; Lindsey, K.; Carr, J.P.; Slabas, A.R. Extracellular ATP is a regulator of pathogen defence in plants. Plant J. 2009, 60, 436–448. [Google Scholar] [CrossRef]
  16. Kim, S.H.; Yang, S.H.; Kim, T.J.; Han, J.S.; Suh, J.W. Hypertonic stress increased extracellular ATP levels and the expression of stress-responsive genes in Arabidopsis thaliana seedlings. Biosci. Biotechnol. Biochem. 2009, 73, 1252–1256. [Google Scholar] [CrossRef] [Green Version]
  17. Sun, J.; Zhang, X.; Deng, S.; Zhang, C.; Wang, M.; Ding, M.; Zhao, R.; Shen, X.; Zhou, X.; Lu, C.; et al. Extracellular ATP signaling is mediated by H2O2 and cytosolic Ca2+ in the salt response of Populus euphratica cells. PLoS ONE 2012, 7, e53136. [Google Scholar] [CrossRef] [Green Version]
  18. Deng, S.; Sun, J.; Zhao, R.; Ding, M.; Zhang, Y.; Sun, Y.; Wang, W.; Tan, Y.; Liu, D.; Ma, X.; et al. Populus euphratica APYRASE2 enhances cold tolerance by modulating vesicular trafficking and extracellular ATP in Arabidopsis plants. Plant Physiol. 2015, 169, 530–548. [Google Scholar] [CrossRef] [Green Version]
  19. Choi, J.; Tanaka, K.; Cao, Y.; Qi, Y.; Qiu, J.; Liang, Y.; Lee, S.Y.; Stacey, G. Identification of a plant receptor for extracellular ATP. Science 2014, 343, 290–294. [Google Scholar] [CrossRef]
  20. Pham, A.Q.; Cho, S.H.; Nguyen, C.T.; Stacey, G. Arabidopsis lectin receptor kinase P2K2 is a second plant receptor for extracellular ATP and contributes to innate immunity. Plant Physiol. 2020, 183, 1364–1375. [Google Scholar] [CrossRef] [PubMed]
  21. Chen, D.; Hao, F.; Mu, H.; Ahsan, N.; Thelen, J.J.; Stacey, G. S-acylation of P2K1 mediates extracellular ATP-induced immune signaling in Arabidopsis. Nat. Commun. 2021, 12, 2750. [Google Scholar] [CrossRef]
  22. Zhu, R.; Dong, X.; Hao, W.; Gao, W.; Zhang, W.; Xia, S.; Liu, T.; Shang, Z. Heterotrimeric G protein-regulated Ca2+ influx and PIN2 asymmetric distribution are involved in Arabidopsis thaliana roots’ avoidance response to extracellular ATP. Front. Plant Sci. 2017, 8, 1522. [Google Scholar] [CrossRef] [Green Version]
  23. Demidchik, V.; Shang, Z.; Shin, R.; Thompson, E.; Rubio, L.; Laohavisit, A.; Mortimer, J.C.; Chivasa, S.; Slabas, A.R.; Glover, B.J.; et al. Plant extracellular ATP signalling by plasma membrane NADPH oxidase and Ca2+ channels. Plant J. 2009, 58, 903–913. [Google Scholar] [CrossRef]
  24. Song, C.J.; Steinebrunner, I.; Wang, X.; Stout, S.C.; Roux, S.J. Extracellular ATP induces the accumulation of superoxide via NADPH oxidases in Arabidopsis. Plant Physiol. 2006, 140, 1222–1232. [Google Scholar] [CrossRef] [Green Version]
  25. Shang, Z.; Laohavisit, A.; Davies, J.M. Extracellular ATP activates an Arabidopsis plasma membrane Ca2+-permeable conductance. Plant Signal. Behav. 2009, 4, 989–991. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  26. Wang, L.M.; Stacey, G.; Leblanc-Fournier, N.; Legue, V.; Moulia, B.; Davies, J.M. Early extracellular ATP signaling in Arabidopsis root epidermis: A multi-conductance process. Front. Plant Sci. 2019, 10, 1064. [Google Scholar] [CrossRef] [PubMed]
  27. Demidchik, V.; Nichols, C.; Oliynyk, M.; Dark, A.; Glover, B.J.; Davies, J.M. Is ATP a signaling agent in plants? Plant Physiol. 2003, 133, 456–461. [Google Scholar] [CrossRef] [Green Version]
  28. Foresi, N.P.; Laxalt, A.M.; Tonon, C.V.; Casalongue, C.A.; Lamattina, L. Extracellular ATP induces nitric oxide production in tomato cell suspensions. Plant Physiol. 2007, 145, 589–592. [Google Scholar] [CrossRef] [Green Version]
  29. Matthus, E.; Sun, J.; Wang, L.M.; Bhat, M.G.; Mohammad-Sidik, A.B.; Wilkins, K.A.; Leblanc-Fournier, N.; Legue, V.; Moulia, B.; Stacey, G.; et al. DORN1/P2K1 and purino-calcium signalling in plants: Making waves with extracellular ATP. Ann. Bot. 2019, 124, 1227–1242. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  30. Holdaway-Clarke, T.L.; Hepler, P.K. Control of pollen tube growth: Role of ion gradients and fluxes. New Phytol. 2003, 159, 539–563. [Google Scholar] [CrossRef]
  31. Steinhorst, L.; Kudla, J. Calcium—A central regulator of pollen germination and tube growth. Biochim. Biophys. Acta 2013, 1833, 1573–1581. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  32. Zheng, R.H.; Su, S.; Xiao, H.; Tian, H.Q. Calcium: A critical factor in pollen germination and tube elongation. Int. J. Mol. Sci. 2019, 20, 420. [Google Scholar] [CrossRef] [Green Version]
  33. Li, D.D.; Guan, H.; Li, F.; Liu, C.Z.; Dong, Y.X.; Zhang, X.S.; Gao, X.Q. Arabidopsis shaker pollen inward K+ channel SPIK functions in SnRK1 complex-regulated pollen hydration on the stigma. J. Integr. Plant. Biol. 2017, 59, 604–611. [Google Scholar] [CrossRef] [Green Version]
  34. Amien, S.; Kliwer, I.; Marton, M.L.; Debener, T.; Geiger, D.; Becker, D.; Dresselhaus, T. Defensin-like ZmES4 mediates pollen tube burst in maize via opening of the potassium channel KZM1. PLoS Biol. 2010, 8, e1000388. [Google Scholar] [CrossRef] [Green Version]
  35. Mouline, K.; Very, A.A.; Gaymard, F.; Boucherez, J.; Pilot, G.; Devic, M.; Bouchez, D.; Thibaud, J.B.; Sentenac, H. Pollen tube development and competitive ability are impaired by disruption of a Shaker K+ channel in Arabidopsis. Genes Dev. 2002, 16, 339–350. [Google Scholar] [CrossRef] [Green Version]
  36. Fan, L.M.; Wang, Y.F.; Wang, H.; Wu, W.H. In vitro Arabidopsis pollen germination and characterization of the inward potassium currents in Arabidopsis pollen grain protoplasts. J. Exp. Bot. 2001, 52, 1603–1614. [Google Scholar] [CrossRef] [Green Version]
  37. Liu, L.; Zheng, C.; Kuang, B.; Wei, L.; Yan, L.; Wang, T. Receptor-like kinase RUPO interacts with potassium transporters to regulate pollen tube growth and integrity in rice. PLoS Genet. 2016, 12, e1006085. [Google Scholar] [CrossRef] [Green Version]
  38. Fan, L.M.; Wu, W.H.; Yang, H.Y. Identification and characterization of the inward K+ channel in the plasma membrane of Brassica pollen protoplasts. Plant Cell Physiol. 1999, 40, 859–865. [Google Scholar] [CrossRef] [Green Version]
  39. Zhao, L.N.; Shen, L.K.; Zhang, W.Z.; Zhang, W.; Wang, Y.; Wu, W.H. Ca2+-dependent protein kinase11 and 24 modulate the activity of the inward rectifying K+ channels in Arabidopsis pollen tubes. Plant Cell 2013, 25, 649–661. [Google Scholar] [CrossRef] [Green Version]
  40. Yang, F.; Wang, T.; Liu, L. Pollen germination is impaired by disruption of a Shaker K+ channel OsAKT1.2 in rice. J. Plant Physiol. 2020, 248, 153140. [Google Scholar] [CrossRef]
  41. Wang, S.S.; Diao, W.Z.; Yang, X.; Qiao, Z.; Wang, M.; Acharya, B.R.; Zhang, W. Arabidopsis thaliana CML25 mediates the Ca2+ regulation of K+ transmembrane trafficking during pollen germination and tube elongation. Plant Cell Environ. 2015, 38, 2372–2386. [Google Scholar] [CrossRef]
  42. Pierson, E.S.; Miller, D.D.; Callaham, D.A.; Shipley, A.M.; Rivers, B.A.; Cresti, M.; Hepler, P.K. Pollen tube growth is coupled to the extracellular calcium ion flux and the intracellular calcium gradient: Effect of BAPTA-type buffers and hypertonic media. Plant Cell 1994, 6, 1815–1828. [Google Scholar]
  43. Malho, R.; Trewavas, A.J. Localized apical increases of cytosolic free calcium control pollen tube orientation. Plant Cell 1996, 8, 1935–1949. [Google Scholar] [CrossRef]
  44. Cole, R.A.; Fowler, J.E. Polarized growth: Maintaining focus on the tip. Curr. Opin. Plant Biol. 2006, 9, 579–588. [Google Scholar] [CrossRef] [PubMed]
  45. Iwano, M.; Entani, T.; Shiba, H.; Kakita, M.; Nagai, T.; Mizuno, H.; Miyawaki, A.; Shoji, T.; Kubo, K.; Isogai, A.; et al. Fine-tuning of the cytoplasmic Ca2+ concentration is essential for pollen tube growth. Plant Physiol. 2009, 150, 1322–1334. [Google Scholar] [CrossRef] [Green Version]
  46. Iwano, M.; Shiba, H.; Miwa, T.; Che, F.S.; Takayama, S.; Nagai, T.; Miyawaki, A.; Isogai, A. Ca2+ dynamics in a pollen grain and papilla cell during pollination of Arabidopsis. Plant Physiol. 2004, 136, 3562–3571. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  47. Rathore, K.S.; Cork, R.J.; Robinson, K.R. A cytoplasmic gradient of Ca2+ is correlated with the growth of lily pollen tubes. Dev. Biol. 1991, 148, 612–619. [Google Scholar] [CrossRef]
  48. Konrad, K.R.; Wudick, M.M.; Feijo, J.A. Calcium regulation of tip growth: New genes for old mechanisms. Curr. Opin. Plant Biol. 2011, 14, 721–730. [Google Scholar] [CrossRef]
  49. Kaya, H.; Nakajima, R.; Iwano, M.; Kanaoka, M.M.; Kimura, S.; Takeda, S.; Kawarazaki, T.; Senzaki, E.; Hamamura, Y.; Higashiyama, T.; et al. Ca2+-activated reactive oxygen species production by Arabidopsis RbohH and RbohJ is essential for proper pollen tube tip growth. Plant Cell 2014, 26, 1069–1080. [Google Scholar] [CrossRef] [Green Version]
  50. Parrotta, L.; Faleri, C.; Guerriero, G.; Cai, G. Cold stress affects cell wall deposition and growth pattern in tobacco pollen tubes. Plant Sci. 2019, 283, 329–342. [Google Scholar] [CrossRef]
  51. Ruan, H.Q.; Li, J.; Wang, T.; Ren, H.Y. Secretory vesicles targeted to plasma membrane during pollen germination and tube growth. Front. Cell Dev. Biol. 2021, 8, 615447. [Google Scholar] [CrossRef] [PubMed]
  52. Battey, N.H.; James, N.C.; Greenland, A.J.; Brownlee, C. Exocytosis and endocytosis. Plant Cell 1999, 11, 643–660. [Google Scholar] [CrossRef] [PubMed]
  53. Camacho, L.; Malho, R. Endo/exocytosis in the pollen tube apex is differentially regulated by Ca2+ and GTPases. J. Exp. Bot. 2003, 54, 83–92. [Google Scholar] [CrossRef] [PubMed]
  54. Zonia, L. Spatial and temporal integration of signalling networks regulating pollen tube growth. J. Exp. Bot. 2010, 61, 1939–1957. [Google Scholar] [CrossRef] [Green Version]
  55. Wang, Y.F.; Fan, L.M.; Zhang, W.Z.; Zhang, W.; Wu, W.H. Ca2+-permeable channels in the plasma membrane of arabidopsis pollen are regulated by actin microfilaments. Plant Physiol. 2004, 136, 3892–3904. [Google Scholar] [CrossRef] [Green Version]
  56. Malho, R.; Liu, Q.; Monteiro, D.; Rato, C.; Camacho, L.; Dinis, A. Signalling pathways in pollen germination and tube growth. Protoplasma 2006, 228, 21–30. [Google Scholar] [CrossRef] [Green Version]
  57. Wu, J.Y.; Jin, C.; Qu, H.Y.; Tao, S.T.; Xu, G.H.; Wu, J.; Wu, H.Q.; Zhang, S.L. Low temperature inhibits pollen viability by alteration of actin cytoskeleton and regulation of pollen plasma membrane ion channels in Pyrus pyrifolia. Environ. Exp. Bot. 2012, 78, 70–75. [Google Scholar] [CrossRef]
  58. Dutta, R.; Robinson, K.R. Identification and characterization of stretch-activated ion channels in pollen protoplasts. Plant Physiol. 2004, 135, 1398–1406. [Google Scholar] [CrossRef] [Green Version]
  59. Frietsch, S.; Wang, Y.F.; Sladek, C.; Poulsen, L.R.; Romanowsky, S.M.; Schroeder, J.I.; Harper, J.F. A cyclic nucleotide-gated channel is essential for polarized tip growth of pollen. Proc. Natl. Acad. Sci. USA 2007, 104, 14531–14536. [Google Scholar] [CrossRef] [Green Version]
  60. Michard, E.; Lima, P.T.; Borges, F.; Silva, A.C.; Portes, M.T.; Carvalho, J.E.; Gilliham, M.; Liu, L.H.; Obermeyer, G.; Feijo, J.A. Glutamate receptor-like genes form Ca2+ channels in pollen tubes and are regulated by pistil D-serine. Science 2011, 332, 434–437. [Google Scholar] [CrossRef] [Green Version]
  61. Wu, Y.; Xu, X.; Li, S.; Liu, T.; Ma, L.; Shang, Z. Heterotrimeric G-protein participation in Arabidopsis pollen germination through modulation of a plasmamembrane hyperpolarization-activated Ca2+-permeable channel. New Phytol. 2007, 176, 550–559. [Google Scholar] [CrossRef]
  62. Wu, J.; Shang, Z.; Wu, J.; Jiang, X.; Moschou, P.N.; Sun, W.; Roubelakis-Angelakis, K.A.; Zhang, S. Spermidine oxidase-derived H2O2 regulates pollen plasma membrane hyperpolarization-activated Ca2+-permeable channels and pollen tube growth. Plant J. 2010, 63, 1042–1053. [Google Scholar] [CrossRef]
  63. Wu, Y.; Qin, B.; Feng, K.; Yan, R.; Kang, E.; Liu, T.; Shang, Z. Extracellular ATP promoted pollen germination and tube growth of Nicotiana tabacum through promoting K+ and Ca2+ absorption. Plant Reprod. 2018, 31, 399–410. [Google Scholar] [CrossRef]
  64. Reichler, S.A.; Torres, J.; Rivera, A.L.; Cintolesi, V.A.; Clark, G.; Roux, S.J. Intersection of two signalling pathways: Extracellular nucleotides regulate pollen germination and pollen tube growth via nitric oxide. J. Exp. Bot. 2009, 60, 2129–2138. [Google Scholar] [CrossRef] [Green Version]
  65. Steinebrunner, I.; Wu, J.; Sun, Y.; Corbett, A.; Roux, S.J. Disruption of apyrases inhibits pollen germination in Arabidopsis. Plant Physiol 2003, 131, 1638–1647. [Google Scholar] [CrossRef] [Green Version]
  66. Zhou, J.H.; Fan, C.Y.; Liu, K.; Jing, Y.P. Extracellular ATP is involved in the initiation of pollen germination and tube growth in Picea meyeri. Trees Struct. Funct. 2015, 29, 563–574. [Google Scholar] [CrossRef]
  67. Clark, G.; Roux, S.J. Apyrases, extracellular ATP and the regulation of growth. Curr. Opin. Plant. Biol. 2011, 14, 700–706. [Google Scholar] [CrossRef] [PubMed]
  68. Demidchik, V.; Shang, Z.; Shin, R.; Colaco, R.; Laohavisit, A.; Shabala, S.; Davies, J.M. Receptor-like activity evoked by extracellular ADP in Arabidopsis root epidermal plasma membrane. Plant Physiol. 2011, 156, 1375–1385. [Google Scholar] [CrossRef] [Green Version]
  69. Jeter, C.R.; Tang, W.; Henaff, E.; Butterfield, T.; Roux, S.J. Evidence of a novel cell signaling role for extracellular adenosine triphosphates and diphosphates in Arabidopsis. Plant Cell 2004, 16, 2652–2664. [Google Scholar] [CrossRef] [Green Version]
  70. Wang, L.M.; Wilkins, K.A.; Davies, J.M. Arabidopsis DORN1 extracellular ATP receptor; activation of plasma membrane K+-and Ca2+-permeable conductances. New Phytol. 2018, 218, 1301–1304. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  71. Bellande, K.; Bono, J.J.; Savelli, B.; Jamet, E.; Canut, H. Plant lectins and Lectin Receptor-Like Kinases: How do they sense the outside? Int. J. Mol. Sci. 2017, 18, 1164. [Google Scholar] [CrossRef]
  72. Wang, F.; Jia, J.; Wang, Y.; Wang, W.; Chen, Y.; Liu, T.; Shang, Z. Hyperpolization-activated Ca2+ channels in guard cell plasma membrane are involved in extracellular ATP-promoted stomatal opening in Vicia faba. J. Plant Physiol. 2014, 171, 1241–1247. [Google Scholar] [CrossRef]
  73. Weerasinghe, R.R.; Swanson, S.J.; Okada, S.F.; Garrett, M.B.; Kim, S.Y.; Stacey, G.; Boucher, R.C.; Gilroy, S.; Jones, A.M. Touch induces ATP release in Arabidopsis roots that is modulated by the heterotrimeric G-protein complex. FEBS Lett. 2009, 583, 2521–2526. [Google Scholar] [CrossRef] [Green Version]
  74. Brost, C.; Studtrucker, T.; Reimann, R.; Denninger, P.; Czekalla, J.; Krebs, M.; Fabry, B.; Schumacher, K.; Grossmann, G.; Dietrich, P. Multiple cyclic nucleotide-gated channels coordinate calcium oscillations and polar growth of root hairs. Plant J. 2019, 99, 910–923. [Google Scholar] [CrossRef] [PubMed]
  75. Moeder, W.; Urquhart, W.; Ung, H.; Yoshioka, K. The role of cyclic nucleotide-gated ion channels in plant immunity. Mol. Plant 2011, 4, 442–452. [Google Scholar] [CrossRef] [PubMed]
  76. Duszyn, M.; Swiezawska, B.; Szmidt-Jaworska, A.; Jaworski, K. Cyclic nucleotide gated channels (CNGCs) in plant signalling-Current knowledge and perspectives. J. Plant. Physiol. 2019, 241, 153035. [Google Scholar] [CrossRef] [PubMed]
  77. Tunc-Ozdemir, M.; Tang, C.; Ishka, M.R.; Brown, E.; Groves, N.R.; Myers, C.T.; Rato, C.; Poulsen, L.R.; McDowell, S.; Miller, G.; et al. A cyclic nucleotide-gated channel (CNGC16) in pollen is critical for stress tolerance in pollen reproductive development. Plant Physiol. 2013, 161, 1010–1020. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  78. Chin, K.; DeFalco, T.A.; Moeder, W.; Yoshioka, K. The Arabidopsis cyclic nucleotide-gated ion channels AtCNGC2 and AtCNGC4 work in the same signaling pathway to regulate pathogen defense and floral transition. Plant Physiol. 2013, 163, 611–624. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  79. Chan, C.W.; Schorrak, L.M.; Smith, R.K., Jr.; Bent, A.F.; Sussman, M.R. A cyclic nucleotide-gated ion channel, CNGC2, is crucial for plant development and adaptation to calcium stress. Plant Physiol. 2003, 132, 728–731. [Google Scholar] [CrossRef] [Green Version]
  80. Katano, K.; Kataoka, R.; Fujii, M.; Suzuki, N. Differences between seedlings and flowers in anti-ROS based heat responses of Arabidopsis plants deficient in cyclic nucleotide gated channel 2. Plant Physiol. Biochem. 2018, 123, 288–296. [Google Scholar] [CrossRef]
  81. Gao, Q.F.; Gu, L.L.; Wang, H.Q.; Fei, C.F.; Fang, X.; Hussain, J.; Sun, S.J.; Dong, J.Y.; Liu, H.; Wang, Y.F. Cyclic nucleotide-gated channel 18 is an essential Ca2+ channel in pollen tube tips for pollen tube guidance to ovules in Arabidopsis. Proc. Natl. Acad. Sci. USA 2016, 113, 3096–3101. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  82. Rahmati Ishka, M.; Brown, E.; Weigand, C.; Tillett, R.L.; Schlauch, K.A.; Miller, G.; Harper, J.F. A comparison of heat-stress transcriptome changes between wild-type Arabidopsis pollen and a heat-sensitive mutant harboring a knockout of cyclic nucleotide-gated cation channel 16 (cngc16). BMC Genom. 2018, 19, 549. [Google Scholar] [CrossRef] [PubMed]
  83. Tunc-Ozdemir, M.; Jones, A.M. Ligand-induced dynamics of heterotrimeric G protein-coupled receptor-like kinase complexes. PLoS ONE 2017, 12, e0171854. [Google Scholar]
  84. Tunc-Ozdemir, M.; Urano, D.; Jaiswal, D.K.; Clouse, S.D.; Jones, A.M. Direct modulation of heterotrimeric G protein-coupled signaling by a receptor kinase complex. J. Biol. Chem. 2016, 291, 13918–13925. [Google Scholar] [CrossRef] [Green Version]
  85. Jia, H.; Song, G.; Werth, E.G.; Walley, J.W.; Hicks, L.M.; Jones, A.M. Receptor-Like kinase phosphorylation of Arabidopsis heterotrimeric G-protein Gα -subunit AtGPA1. Proteomics 2019, 19, e1900265. [Google Scholar] [CrossRef]
  86. Urano, D.; Chen, J.G.; Botella, J.R.; Jones, A.M. Heterotrimeric G protein signalling in the plant kingdom. Open Biol. 2013, 3, 120186. [Google Scholar] [CrossRef] [Green Version]
  87. Very, A.A.; Davies, J.M. Hyperpolarization-activated calcium channels at the tip of Arabidopsis root hairs. Proc. Natl. Acad. Sci. USA 2000, 97, 9801–9806. [Google Scholar] [CrossRef] [Green Version]
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Figure 1. ATP-regulated PG and PTG in various plant species. Pollen grains of 34 plant species were germinated in vitro in the medium containing 18% sucrose, 0.1 mM KCl, and 0.5% agarose. Germination duration of each species is listed in Table 1. PG (A) and PTG (B) were noted. In each experiment, at least 300 pollen grains or 150 pollen tubes were counted or measured. Data from 3 replicates were calculated to obtain mean ± SD. Student’s t-test p values: * p < 0.05, ** p < 0.01.
Figure 1. ATP-regulated PG and PTG in various plant species. Pollen grains of 34 plant species were germinated in vitro in the medium containing 18% sucrose, 0.1 mM KCl, and 0.5% agarose. Germination duration of each species is listed in Table 1. PG (A) and PTG (B) were noted. In each experiment, at least 300 pollen grains or 150 pollen tubes were counted or measured. Data from 3 replicates were calculated to obtain mean ± SD. Student’s t-test p values: * p < 0.05, ** p < 0.01.
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Figure 2. eATP regulates the PG and PTG of Arabidopsis thaliana by facilitating K+ uptake. Apyrase-inhibited PG (A) and PTG (D), ATP-regulated PG (B), and PTG (E) in medium containing serial concentrations of KCl. K+ channel blockers (1 mM) inhibited ATP-promoted PG (C) and PTG (F). In (A–F), the K+ concentration in the medium is 0.1 mM. In each experiment, at least 300 pollen grains were counted to obtain PG, and at least 150 pollen tubes were measured to obtain the pollen tube length. Data from 3 replicates were combined to obtain the mean ± SD. Student’s t test p values: * p < 0.05, ** p < 0.01.
Figure 2. eATP regulates the PG and PTG of Arabidopsis thaliana by facilitating K+ uptake. Apyrase-inhibited PG (A) and PTG (D), ATP-regulated PG (B), and PTG (E) in medium containing serial concentrations of KCl. K+ channel blockers (1 mM) inhibited ATP-promoted PG (C) and PTG (F). In (A–F), the K+ concentration in the medium is 0.1 mM. In each experiment, at least 300 pollen grains were counted to obtain PG, and at least 150 pollen tubes were measured to obtain the pollen tube length. Data from 3 replicates were combined to obtain the mean ± SD. Student’s t test p values: * p < 0.05, ** p < 0.01.
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Figure 3. eATP regulates PG and PTG of Arabidopsis thaliana by facilitating Ca2+ uptake. ATP (0.1 mM) regulates PG (A) and PTG (B) in medium containing a Ca2+ chelator, serial concentrations of Ca2+, and channel blockers (0.1 mM). In each experiment, at least 300 pollen grains were counted to obtain PG, and at least 150 pollen tubes were measured to obtain the pollen tube length. Data from 3 replicates were combined to obtain the mean ± SD. Student’s t test p values: * p < 0.05, ** p < 0.01.
Figure 3. eATP regulates PG and PTG of Arabidopsis thaliana by facilitating Ca2+ uptake. ATP (0.1 mM) regulates PG (A) and PTG (B) in medium containing a Ca2+ chelator, serial concentrations of Ca2+, and channel blockers (0.1 mM). In each experiment, at least 300 pollen grains were counted to obtain PG, and at least 150 pollen tubes were measured to obtain the pollen tube length. Data from 3 replicates were combined to obtain the mean ± SD. Student’s t test p values: * p < 0.05, ** p < 0.01.
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Figure 4. CsCl inhibits eATP-stimulated K+ influx in the protoplasts of Arabidopsis pollen grains. (A) CsCl (1 mM) inhibited resting and 0.1 mM ATP-stimulated inward K+ currents. Representative current traces from step-voltage clamping are shown. (B,C) I-V relationship curves of inward K+ currents (n = 7). In each experiment, data from 7 protoplasts were recorded and combined to obtain the mean ± SD.
Figure 4. CsCl inhibits eATP-stimulated K+ influx in the protoplasts of Arabidopsis pollen grains. (A) CsCl (1 mM) inhibited resting and 0.1 mM ATP-stimulated inward K+ currents. Representative current traces from step-voltage clamping are shown. (B,C) I-V relationship curves of inward K+ currents (n = 7). In each experiment, data from 7 protoplasts were recorded and combined to obtain the mean ± SD.
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Figure 5. GdCl3 inhibits eATP-stimulated Ca2+ influx in the protoplasts of Arabidopsis pollen grain. (A) GdCl3 (0.1 mM) inhibited resting and 0.1 mM ATP-stimulated inward Ca2+ currents. Representative current traces from step-voltage clamping are shown. (B,C) I-V relationship curves of the inward Ca2+ currents (n = 7). In each experiment, data from 7 protoplasts were recorded and combined to obtain the mean ± SD.
Figure 5. GdCl3 inhibits eATP-stimulated Ca2+ influx in the protoplasts of Arabidopsis pollen grain. (A) GdCl3 (0.1 mM) inhibited resting and 0.1 mM ATP-stimulated inward Ca2+ currents. Representative current traces from step-voltage clamping are shown. (B,C) I-V relationship curves of the inward Ca2+ currents (n = 7). In each experiment, data from 7 protoplasts were recorded and combined to obtain the mean ± SD.
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Figure 6. P2K1 receptor (DORN1) is involved in the eATP-regulated PG, PTG, and ion influx. Two DORN1 null mutants (dorn1-1, dorn1-3) were used. (A–D) show the effects of ATP on PG (A) and PTG (B) in medium containing 0.1 mM KCl and the corresponding K+ influx current traces (C) and I-V relationship curves ((D), n = 7). (E–H) show the effect of ATP on PG (E) and PTG (F) in medium containing 0.1 mM CaCl2 and the corresponding Ca2+ influx current traces (G) and I-V relationship curves ((H), n = 7). In the pollen germination experiment, at least 300 pollen grains or 150 pollen were counted or measured; data from 3 replicates were combined to obtain the mean ± SD. Student’s t test p values: * p < 0.05, ** p < 0.01. In the patch clamp experiment, data from 7 pollen protoplasts were recorded and combined to obtain the mean ± SD.
Figure 6. P2K1 receptor (DORN1) is involved in the eATP-regulated PG, PTG, and ion influx. Two DORN1 null mutants (dorn1-1, dorn1-3) were used. (A–D) show the effects of ATP on PG (A) and PTG (B) in medium containing 0.1 mM KCl and the corresponding K+ influx current traces (C) and I-V relationship curves ((D), n = 7). (E–H) show the effect of ATP on PG (E) and PTG (F) in medium containing 0.1 mM CaCl2 and the corresponding Ca2+ influx current traces (G) and I-V relationship curves ((H), n = 7). In the pollen germination experiment, at least 300 pollen grains or 150 pollen were counted or measured; data from 3 replicates were combined to obtain the mean ± SD. Student’s t test p values: * p < 0.05, ** p < 0.01. In the patch clamp experiment, data from 7 pollen protoplasts were recorded and combined to obtain the mean ± SD.
Plants 10 01743 g006
Plants 10 01743 g007 550
Figure 7. Heterotrimeric G protein α subunit (GPA1) is involved in eATP-regulated PG, PTG, and ion influx. Two GPA1 null mutants (gpa1-1, gpa1-2) were used. (A–D) show the effects of ATP on PG (A) and PTG (B) in medium containing 0.1 mM KCl with corresponding K+ influx current traces (C) and I-V relationship curves ((D), n = 7). E–H show the effects of ATP on PG (E) and PTG (F) in medium containing 0.1 mM CaCl2 with corresponding Ca2+ influx current traces (G) and I-V relationship curves ((H), n = 7). In the pollen germination experiment, at least 300 pollen grains or 150 pollen were counted or measured; data from 3 replicates were combined to obtain the mean ± SD. Student’s t test p values: * p < 0.05. In the patch clamp experiment, data from at least 7 pollen protoplasts were recorded and combined to obtain the mean ± SD.
Figure 7. Heterotrimeric G protein α subunit (GPA1) is involved in eATP-regulated PG, PTG, and ion influx. Two GPA1 null mutants (gpa1-1, gpa1-2) were used. (A–D) show the effects of ATP on PG (A) and PTG (B) in medium containing 0.1 mM KCl with corresponding K+ influx current traces (C) and I-V relationship curves ((D), n = 7). E–H show the effects of ATP on PG (E) and PTG (F) in medium containing 0.1 mM CaCl2 with corresponding Ca2+ influx current traces (G) and I-V relationship curves ((H), n = 7). In the pollen germination experiment, at least 300 pollen grains or 150 pollen were counted or measured; data from 3 replicates were combined to obtain the mean ± SD. Student’s t test p values: * p < 0.05. In the patch clamp experiment, data from at least 7 pollen protoplasts were recorded and combined to obtain the mean ± SD.
Plants 10 01743 g007
Plants 10 01743 g008 550
Figure 8. CNGC2 and CNGC4 are involved in eATP-regulated PG, PTG, and ion influx. Two CNGCs null mutants (cngc2, cngc4) were used. (A–D) show the effects of ATP on PG (A) and PTG (B) in medium containing 0.1 mM KCl with corresponding K+ influx current traces (C) and I-V relationship curves ((D), n = 7). (E–H) show the effects of ATP on PG (E) and PTG (F) in medium containing 0.1 mM CaCl2 with corresponding Ca2+ influx current traces (G) and I-V relationship curves ((H), n = 7). In the pollen germination experiment, at least 300 pollen grains or 150 pollen were counted or measured; data from 3 replicates were combined to obtain the mean ± SD. Student’s t test p values: * p < 0.05, ** p < 0.01. In the patch clamp experiment, data from at least 7 pollen protoplasts were recorded and combined to obtain the mean ± SD.
Figure 8. CNGC2 and CNGC4 are involved in eATP-regulated PG, PTG, and ion influx. Two CNGCs null mutants (cngc2, cngc4) were used. (A–D) show the effects of ATP on PG (A) and PTG (B) in medium containing 0.1 mM KCl with corresponding K+ influx current traces (C) and I-V relationship curves ((D), n = 7). (E–H) show the effects of ATP on PG (E) and PTG (F) in medium containing 0.1 mM CaCl2 with corresponding Ca2+ influx current traces (G) and I-V relationship curves ((H), n = 7). In the pollen germination experiment, at least 300 pollen grains or 150 pollen were counted or measured; data from 3 replicates were combined to obtain the mean ± SD. Student’s t test p values: * p < 0.05, ** p < 0.01. In the patch clamp experiment, data from at least 7 pollen protoplasts were recorded and combined to obtain the mean ± SD.
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Table
Table 1. Plant materials for in vitro pollen germination (sorted by the initials of the Latin names of plant species).
Table 1. Plant materials for in vitro pollen germination (sorted by the initials of the Latin names of plant species).
Latin NameFamilyClassPhylumGermination Duration (min)
1Aquilegia viridifloraRanunculaceaeDicotyledoneaeAngiospermae30
2Arabidopsis thalianaBrassicaceaeDicotyledoneaeAngiospermae300
3Berberis thunbergiiBerberidaceaeDicotyledoneaeAngiospermae40
4Brassica campestrisBrassicaceaeDicotyledoneaeAngiospermae240
5Brassica pekinensisBrassicaceaeDicotyledoneaeAngiospermae150
6Cercis chinensisLeguminosaeDicotyledoneaeAngiospermae90
7Clivia miniataAmaryllidaceaeMonocotyledoneaeAngiospermae420
8Cotinus coggygriaAnacardiaceaeDicotyledoneaeAngiospermae40
9Cotoneaster horizontalisRosaceaeDicotyledoneaeAngiospermae60
10Forsythia suspensaOleaceaeDicotyledoneaeAngiospermae120
11Hyacinthus orientalisHyacinthaceaeMonocotyledoneaeAngiospermae80
12Jasminum nudiflorumOleaceaeDicotyledoneaeAngiospermae90
13Kolkwitzia amabilisCaprifoliaceaeDicotyledoneaeAngiospermae60
14Lonicera maackiiCaprifoliaceaeDicotyledoneaeAngiospermae60
15Lonicera japonicaCaprifoliaceaeDicotyledoneaeAngiospermae120
16Magnolia denudataMagnoliaceaeDicotyledoneaeAngiospermae2880
17Malus hallianaRosaceaeDicotyledoneaeAngiospermae30
18Malus micromalusRosaceaeDicotyledoneaeAngiospermae60
19Nicotiana tabacumSolanaceaeDicotyledoneaeAngiospermae30
20Orychophragmus violaceusBrassicaceaeDicotyledoneaeAngiospermae180
21Paeonia suffruticosaPaeoniaceaeDicotyledoneaeAngiospermae60
22Paeonia lactifloraPaeoniaceaeDicotyledoneaeAngiospermae60
23Paulownia fortuneiScrophulariaceaeDicotyledoneaeAngiospermae60
24Pinus bungeanaPinaceaeConiferopsidaGymnosperm4320
25Pinus tabulaeformisPinaceaeConiferopsidaGymnosperm4320
26Punica granatumPunicaceaeDicotyledoneaeAngiospermae120
27Prunus cerasiferaRosaceaeDicotyledoneaeAngiospermae60
28Rosa xanthinaRosaceaeDicotyledoneaeAngiospermae20
29Robinia pseudoacaciaLeguminosaeDicotyledoneaeAngiospermae30
30Rosa farreriRosaceaeDicotyledoneaeAngiospermae30
31Saintpaulia ionanthaGesneriaceaeDicotyledoneaeAngiospermae180
32Sophora japonicaLeguminosaeDicotyledoneaeAngiospermae30
33Swida albaCorneceaeDicotyledoneaeAngiospermae60
34Syringa oblataOleaceaeDicotyledoneaeAngiospermae90
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Wu, Y.; Yin, H.; Liu, X.; Xu, J.; Qin, B.; Feng, K.; Kang, E.; Shang, Z. P2K1 Receptor, Heterotrimeric Gα Protein and CNGC2/4 Are Involved in Extracellular ATP-Promoted Ion Influx in the Pollen of Arabidopsis thaliana. Plants 2021, 10, 1743. https://doi.org/10.3390/plants10081743

AMA Style

Wu Y, Yin H, Liu X, Xu J, Qin B, Feng K, Kang E, Shang Z. P2K1 Receptor, Heterotrimeric Gα Protein and CNGC2/4 Are Involved in Extracellular ATP-Promoted Ion Influx in the Pollen of Arabidopsis thaliana. Plants. 2021; 10(8):1743. https://doi.org/10.3390/plants10081743

Chicago/Turabian Style

Wu, Yansheng, Hongmin Yin, Xinyue Liu, Jiawei Xu, Baozhi Qin, Kaili Feng, Erfang Kang, and Zhonglin Shang. 2021. "P2K1 Receptor, Heterotrimeric Gα Protein and CNGC2/4 Are Involved in Extracellular ATP-Promoted Ion Influx in the Pollen of Arabidopsis thaliana" Plants 10, no. 8: 1743. https://doi.org/10.3390/plants10081743

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