Gibberellins (GAs) are plant hormones that promote a wide range of developmental processes. While GA signalling is well understood, little is known about how GA is transported or how GA distribution is regulated. Here we utilize fluorescently labelled GAs (GA-Fl) to screen for Arabidopsis mutants deficient in GA transport. We show that the NPF3 transporter efficiently transports GA across cell membranes in vitro and GA-Fl in vivo. NPF3 is expressed in root endodermis and repressed by GA. NPF3 is targeted to the plasma membrane and subject to rapid BFA-dependent recycling. We show that abscisic acid (ABA), an antagonist of GA, is also transported by NPF3 in vitro. ABA promotes NPF3 expression and GA-Fl uptake in plants. On the basis of these results, we propose that GA distribution and activity in Arabidopsis is partly regulated by NPF3 acting as an influx carrier and that GA–ABA interaction may occur at the level of transport.
Unlike animals, plants are sessile organisms that must integrate biotic and abiotic stimuli with their genetic programme to grow and reproduce in a dynamic environment. Growth and development are regulated in response to environmental inputs such as temperature, nutrient status, water, pathogens and light. To enable signal integration, plants employ hormone systems that are exquisitely controlled at multiple levels such as hormone biosynthesis, metabolism, perception and signalling1,2,3. In addition, the distribution and cellular concentration of plant hormones are regulated, thereby enabling highly coordinated cellular responses4,5,6,7,8,9. For example, the combined activities of auxin influx and efflux carrier proteins generate local hormone maxima, minima and auxin gradients that are required for various developmental processes10,11. The recent identification of abscisic acid (ABA), strigolactone and cytokinin transporters6,7,8,9,12 implies that, like auxin, the in planta distribution of these and possibly also other hormones is determined by transporters.
Gibberellins (GAs) are tetracyclic diterpenoid hormones that control many developmental processes such as seed germination, root and shoot elongation, flowering and fruit patterning. The genetic or agrochemical manipulation of GA biosynthesis or signalling is a widespread practice in agriculture. The best-known examples are the dwarfing alleles of wheat REDUCED HEIGHT1 and rice SEMIDWARF1 that are one of the foundations of the so-called ‘Green Revolution’ and resulted in enormous increases in global crop yields after World War II13. Whereas research over the past 15 years has elucidated the GA biosynthetic and signalling pathways at the molecular level, it remains to be determined precisely where GAs are active within the plant and how GAs are transported from sites of synthesis to sites of action. Studies using radiolabelled GA and grafting experiments with GA mutants, have demonstrated that GAs are mobile hormones and that their movement is essential for proper plant growth14,15,16,17,18,19. A recent Arabidopsis grafting experiment with a variety of GA biosynthetic mutants demonstrated long-distance transport of the inactive GA12 (ref. 20). Many GAs are membrane permeable weak acids that can accumulate in the cytoplasm due to an ion-trapping mechanism21. To explain how GAs can pass through the plasma membrane as a part of cell-to-cell transport, the existence of active GA carriers has been proposed22.
We have recently explored the in planta distribution of several bioactive GAs in Arabidopsis thaliana roots using custom-made fluorescein-tagged (fluorescent) GA molecules (GA-Fls)23. Interestingly, these biologically active GA-Fls specifically accumulated in the endodermal cells of the root elongation zone but not in the meristematic or differentiation zones, whereas free fluorescein was detected in all tissues23. The data suggest that the specific accumulation of GA-Fl in the endodermis is tightly regulated23,24. However, the identity of GA transporters involved in this process has remained elusive.
Here we describe a search for GA transporters by screening for mutants defective in GA-Fl accumulation. We show that mutants lacking NPF3, a poorly characterized member of the NPF family, are deficient in the uptake of fluorescent GA into elongating root endodermal cells. NPF3 overexpression causes a striking accumulation of GA-Fl in all root cells and dramatic inhibition of root and shoot growth. Experiments in Xenopus oocytes show that NPF3 is an active GA importer. We also demonstrate that NPF3 transports ABA in oocytes, suggesting that ABA and GA transport may be linked through the dual specificity of several NPF transporters.
NPF3 transports GA-Fl into elongating root endodermal cells
To identify putative GA transporters, we screened a collection of ≈180 transfer DNA (T-DNA) insertion mutants of the ATP-binding cassette and the NITRATE TRANSPORTER1/PEPTIDE TRANSPORTER (NPF) transporter family members for seedlings that were defective in GA-Fl accumulation in the root endodermis25,26 (Supplementary Data 1). Members of both transporter families have been shown to function as plant hormone transporters6,8,9,12,27,28,29,30. The screen was performed visually by testing 10 seedlings per T-DNA line using the confocal microscope. The screen identified a T-DNA line that was deficient in the accumulation of GA-Fl. The T-DNA insertion disrupted NPF3 (At1g68570, NPF3.1), a poorly characterized member of the NPF gene family (Fig. 1a)31,32. Two independent insertion mutants, npf3-1 (SALK_130095) and npf3-2 (GK-356G08) (Fig. 1b), accumulated very low levels of GA3-Fl and GA4-Fl in the elongating endodermal cells compared with the wild-type (WT) but accumulated normal levels of free Fl (Fig. 1c, Supplementary Fig. 1a). Reverse transcription–PCR (RT–PCR) experiments indicated that some regions of the NPF3 transcript accumulated to high levels in the T-DNA lines (Supplementary Fig. 1b,d–e); however, neither allele generated full-length NPF3 RNA (Supplementary Fig. 1b–c). Both T-DNA lines were backcrossed to Col-0. Genetic analysis revealed that the uptake defect segregated as a single recessive mutation completely linked to the insert (n=100). These results suggest that NPF3 may be involved in GA transport into the elongating endodermal cells of the root.
NPF3 belongs to an evolutionarily conserved but strongly expanded and diversified family of transporters with 53 members in Arabidopsis. Arabidopsis NPF1.1 and NPF4.6/AIT1 transport auxin and ABA, respectively12,30. Recent work showed that various NPF proteins can transport GA, ABA and jasmonic acid-isoleucine (JA-Ile)33,34. NPF3 is conserved in all plant lineages and its orthologs share a high degree of identity26, suggesting a fundamental physiological role. Since loss of NPF3 function abolished GA3-Fl accumulation in the elongating endodermal cells we hypothesized that misexpressing NPF3 in additional cell types would affect GA3-Fl accumulation in the root. We introduced a construct into Col-0 plants in which NPF3 was fused to yellow fluorescent protein (YFP) and placed under the control of the 35S promoter (p35S:NPF3-YFP). NPF3 RNA levels were 16- and 5-fold higher (depending on the line) in p35S:NPF3-YFP plants compared with WT plants (Supplementary Fig. 1d). Indeed, accumulation of GA3-Fl was markedly enhanced in these lines (Fig. 1c). This result strongly supports the hypothesis that NPF3 facilitates GA transport in planta. Overexpression of the NPF3 gene in reverse orientation (p35S:NPF3-antisense) resulted in two and threefold reduction (depending on the line) in NPF3 transcript levels compared with WT (Supplementary Fig. 1d) and in reduced GA3-Fl accumulation in elongating endodermis (Fig. 1c). Overall, the results indicate that NPF3 is required for accumulation of GA3-Fl in endodermal cells in the root elongation zone.
NPF3 localization and regulation
Our results suggest that NPF3 is a GA transporter. Indeed, in silico analysis predicts a putative 12 transmembrane domain carrier protein (Supplementary Fig. 2a). Plant hormone transporters localize to the plasma membrane7,8,9,29,35,36, as well as intracellular compartments such as the endoplasmic reticulum and vacuole37,38,39. To address NPF3 subcellular localization, we utilized our p35S:NPF3-YFP lines. Confocal microscopy of p35S:NPF3-YFP root tips showed that NPF3 localizes to the plasma membrane and intracellular membrane compartments (Fig. 2a). By imaging NPF3-YFP in root tip cells where the vacuoles are small and by using chemical and genetic markers that stain the tonoplast and plasma membrane, we were able to rule out vacuolar localization (Fig. 2b and Supplementary Fig. 2b). These results seemingly contradict previous experiments involving transient expression in tobacco that suggested localization of NPF3 orthologs from cucumber (CsNitr1-L, CsNPF3.2) to chloroplasts32. Moreover, in silico analysis showed that the N terminus of Arabidopsis NPF3 lacks a chloroplast targeting sequence that is predicted for CsNitr1-L31. To further investigate NPF3 trafficking to the plasma membrane, we treated p35S:NPF3-YFP seedlings with Brefeldin A (BFA), an inhibitor of ARF–GTP exchange factors, for 15 min and imaged NPF3-YFP by confocal microscopy. This treatment resulted in the depletion of NPF3-YFP from the plasma membrane and accumulation of the transporter in intracellular vesicles, indicating that NPF3 is rapidly targeted to the plasma membrane in a BFA-dependent manner (Fig. 2c). Consistent with this, we observed that BFA-treated roots are deficient in GA3-Fl uptake (Fig. 2d). Thus, NPF3 localization on the plasma membrane is required for GA3-Fl accumulation in the elongating endodermal cells. Co-treatments of p35S:NPF3-YFP seedlings with GA or paclobutrazol (paclo; an inhibitor of GA synthesis) with and without BFA did not show a significant difference compared with respective control treatments, implying that NPF3 subcellular localization or its BFA sensitivity are not directly affected by GA4 levels (Supplementary Fig. 2c-d).
According to published root cell-specific transcriptomic data40 and other publicly available microarray data, NPF3 is expressed in roots, albeit at very low levels. Interestingly, a high-resolution root spatiotemporal microarray expression map shows NPF3 transcripts at higher levels in the root endodermis compared with other tissues in roots (Fig. 2e)40. Moreover, additional support for endodermis localization of NPF3 was obtained by analysing cell type-specific expression data (Supplementary Fig. 3a) derived from microarray studies of RNA bound to ribosomes, which were immunoprecipitated by the use of epitope-tagged ribosomal protein from seedlings41. In combination, the localization of NPF3 transcripts and translation are consistent with a role for NPF3 in GA-Fl accumulation in the root endodermis.
Several plant hormone transporters are regulated at the transcriptional level by their hormone substrate8,37,42. To evaluate the response of NPF3 to GA, we analysed NPF3 transcript abundance following GA treatment. Ten-day-old Col-0 seedlings pretreated with paclo show strongly reduced NPF3 RNA levels in response to 10 μM GA4 treatment as measured by quantitative PCR experiments (Fig. 2f). In agreement, pNPF3:LUC (luciferase) 10-day-old seedlings treated with 10 μM GA3 for 1–24 h showed reduced LUC signal (Fig. 2g). These results indicate that high levels of GA repress NPF3 expression and thus inhibit GA uptake. Published data show that NPF3 is induced by ABA (10 μM, 3 h) and salt stress (150 mM, 12 h)43,44,45. These results were reproduced for ABA in our quantitative PCR experiments (Supplementary Fig. 4a). Accordingly, we show that GA3-Fl accumulation in the endodermis is induced by ABA and NaCl treatments in a concentration-dependent manner (Supplementary Fig. 4b). The ABA induced GA3-Fl uptake into the elongating endodermal cells does not take place in npf3-1 mutant, and therefore is NPF3 dependent (Supplementary Fig. 4b).
NPF3 loss and gain-of-function growth phenotypes
The fluorescent GA experiments suggested that NPF3 is involved in bioactive GA transport in the root. To study NPF3 regulation in GA-mediated plant growth and development, we compared WT, NPF3 loss of function and overexpression lines (p35S:NPF3-YFP), assessing GA-mediated traits such as germination, root and shoot elongation and flowering time. Both npf3-1 and npf3-2 mutants lines were like the WT with respect to all these traits (Fig. 3a,b) despite their failure to accumulate the fluorescently tagged hormone. The lack of a mutant phenotype in the npf3 mutants despite the strong effect on GA-Fl uptake is puzzling. It is possible that there are alternative functionally redundant GA transporters that compensate in the absence of NPF3. This hypothesis is supported by functional transport experiments described below (Fig. 4e,f, Supplementary Fig. 6).
In contrast, p35S:NPF3-YFP plants exhibit delayed germination, decreased hypocotyl growth, and a strong reduction in root and shoot growth (Fig. 3a,b, Supplementary Fig. 5). These defects are similar to those seen in GA-deficient plants46,47. The growth inhibition caused by NPF3 overexpression might be caused by the retention of GA at sites of synthesis, thus preventing movement of GA to key growth sites. If this is correct, one might expect stronger accumulation of GA-Fl in the outer layers (GA-Fl is applied exogenously) for p35S:NPF3-YFP roots. Indeed, GA3-Fl accumulated at higher levels in the epidermal layer compared with the inner layers (Fig. 3c), suggesting that the epidermal layer has imported GA3-Fl and trapped the molecule in the cell in a NPF3-dependent manner. In addition, expression of the GA2ox1 gene, encoding a GA-inactivating enzyme, was transiently reduced in response to GA compared with WT (Supplementary Fig. 5c). The striking ectopic GA-Fl accumulation in additional cells of p35S:NPF3-YFP seedlings, accompanied by GA-related developmental defects observed in these lines, support a role for NPF3 in GA responses.
To further understand the role of NPF3 in GA-mediated root growth, we examined the response of NPF3 loss- and gain-of-function lines to paclo and applied GA. Paclo is an inhibitor of GA synthesis that causes reduced root growth that can be rescued by applying exogenous bioactive GA. The npf3 mutants responded to paclo and applied GA like WT. In comparison, p35S:NPF3-YFP and p35S:NPF3-antisense plants showed a reduced growth response to GA. (Fig. 3d). The response of p35S:NPF3-YFP seedlings to GA is consistent with the hypothesis that ectopic expression of NPF3 inhibits bioactive GA movement to key growth sites. p35S:NPF3-antisense lines showed reduced NPF3 expression (Supplementary Fig. 1d), while no additional change in expression level could be detected in other family members that were shown to transport GA in yeast assays33, and are expressed in the root tip (Supplementary Figs 5d, 6b).
Long-term treatment of p35S:NPF3-YFP lines with GA might compensate for the altered distribution of endogenous hormone. In agreement, long-term (10 and 21 days) GA treatment of the p35S:NPF3-YFP line promoted shoot growth and flowering, largely rescuing the hypocotyl elongation, (depending on NPF3 overexpression strong/weak line; Fig. 3e,f), while partially rescuing the root growth phenotype (once a day for 4 days, 1 μl application, 5 μM GA3 to root tip, in paclo background; Fig. 3d). To investigate whether NPF3 promotes GA activity as opposed to GA storage and degradation, p35S:NPF3-YFP seedlings were grown on increasing concentrations of GA. While WT plants showed reduced growth and yellow shoot colour on high GA concentration (50 μM), p35S:NPF3-YFP showed similar phenotypes when grown on 15 μM GA (Supplementary Fig. 5e). This result suggests that NPF3 promotes accumulation of GA in GA responding cells and that NPF3 is involved in GA-mediated plant growth and development.
Recent work showed that various NPF proteins can transport ABA and nitrate26. To test the role of NPF3 in ABA and nitrate response, we tested NPF3 overexpression lines, T-DNA mutants and antisense lines on ABA and nitrate assays. We could not detect any difference to the WT in response to nitrate for any of the tested lines (Supplementary Fig. 5g–h). However, overexpression of NPF3 resulted in a significant reduction in germination with and without ABA treatment (Supplementary Fig. 5i). Interestingly, we observed a small but significant decrease in germination in the npf3-2 mutant allele and NPF3 antisense line at high ABA concentrations (3 μM; Supplementary Fig. 5i). NPF3 overexpression but not npf3 loss-of-function lines showed significant root response to ABA compared with WT (Supplementary Fig. 5j). It is, therefore, likely that the strong NPF3 overexpression phenotype is driven by the mislocalization of both hormones. These results together with the results showing that ABA induces NPF3 expression and GA-Fl accumulation in the elongating endodermal cells, suggest that NPF3 may be involved in ABA localization and response.
NPF3 is a GA transporter
Our results indicate that NPF3 transports GA-Fl in planta. To elucidate the mechanisms underlying GA transport by NPF3, we used the Xenopus oocyte expression system. Uptake experiments showed that NPF3 mediated GA3-Fl uptake into oocytes (Fig. 4a), confirming that NPF3 is a GA-Fl importer. In contrast, the glucosinolate transporter 2 (NPF2.11/GTR2) and non-expressing control oocytes did not import GA3-Fl into oocytes (Fig. 4a). Oocytes expressing NPF3 exposed to 100 μM GA3 at pH 5 (∼apoplastic pH conditions) showed a 19.1-fold increase in GA3 uptake compared with non-injected oocytes, and 10-fold higher than GTR2 uptake (Fig. 4b), indicating that NPF3 can transport native GA. To determine whether NPF3 transports other active GAs present in plants, we exposed NPF3-expressing oocytes to 100 μM GA1, GA3 or GA4 at pH 5.5 and 7.5. Oocytes expressing NPF3 accumulated ∼14 fold higher GA4 levels compared to GA3, and ∼7 fold higher levels compared to GA1 at pH 5.5 (Fig. 4c). This indicates that GA4, which is the active endogenous GA in Arabidopsis is the preferred GA substrate of NPF3 (Fig. 4c). Most NPF importers characterized to date are proton symporters that utilize the inwardly directed electrochemical proton gradient (ΔμH+) between the plant apoplast (∼pH 5) and cytoplasm (∼pH 7.5) to drive import of substrates48. Oocytes expressing NPF3 showed an increased uptake of GA4, GA3 and GA1 at pH 5.5 compared with pH 7.5 (Fig. 4c). This indicates that transport by NPF3 is dependent on the pH gradient. In agreement, seedlings exposed to pH 7.5 media showed reduced accumulation of GA3-Fl in the root elongation zone compared with roots growing in pH 5.7 media (Fig. 4d,e).
We exposed NPF3-expressing oocytes to increasing concentrations of GA4 and calculated the GA4 transported by NPF3 into the oocytes following 60 min incubation by subtracting uptake in non-injected oocytes (diffusion). This yielded a saturation curve from which we estimate an apparent Km of NPF3 towards GA4 of 0.5 mM (Supplementary Fig. 6a). Kinetic uptake assays of weak acids are, however, notoriously difficult to interpret. The propensity of weak acids to diffuse across cellular membranes at acidic pH and the cumulative nature of the uptake assays makes it difficult to accurately estimate the apparent Km. As an example, we previously estimated the apparent Km value for glucosinolate uptake by GTR2 using liquid chromatography mass spectrometry (LC-MS) and electrophysiology-based uptake assays. LC-MS-based uptake assays estimated a Km value that was approximately fivefold higher (unpublished data) compared with the more accurate value determined by electrophysiology49. We thus judge that the Km of NPF3 towards GA4 is likely to be an overestimation.
It was recently reported that a large number of NPF transporters promote GA uptake in yeast when utilizing a GA-dependent yeast two-hybrid protein–protein interaction approach33. Besides NPF3, six of the apparent GA-importing NPF genes were expressed in different tissues in the root tip. These include NPF2.3, NPF2.10/GTR1, NPF4.1/AIT3, NPF4.2/AIT4, NPF5.6 and NPF5.7 (Supplementary Fig. 6b). Using the Xenopus oocyte system, we compared the ability of NPF3 and the three transporters NPF2.10, NPF4.1 and NPF5.7 to import GA3-Fl and GA4-FI. Interestingly, NPF3 displayed transport activity towards GA3-Fl and GA4-Fl whereas the other genes imported neither of the labelled GA species significantly above levels detected in control oocytes (Fig. 4e). We then tested the ability of the four transporters to import non-conjugated GA3 and GA4. In contrast to the qualitative evidence for GA import provided previously33, only NPF3 and NPF4.1 imported GA3 and GA4 into the oocytes to levels significantly above those found in control oocytes (Fig. 4f). This indicates that the number of putative GA transporters suggested previously33,34 may be an overestimation. Interestingly, NPF4.1 imported GA3, (exogenous to Arabidopsis) to fivefold higher levels compared with NPF3, whereas import of GA4 (endogenous to Arabidopsis) was similar between the two proteins (Fig. 4f). Taken together, these results highlight that before identification and characterization of the transporters, caution must be taken when using fluorescent labelling to follow phytohormone mobility in planta. In this study, application of GA-Fl helped us identify NPF3 as a putative GA transporter but also indicated that NPF3 was solely responsible for GA accumulation in root endodermis. In fact, biochemical characterization shows that NPF4.1 likely acts redundantly and may compensate for NPF3 loss of function in planta.
As the NPF family of transporters possesses a remarkably wide substrate specificity26, we performed competition experiments using known substrates of the family. GA4 import by NPF3 and NPF4.1 was competed with 15-fold excess concentration of NO3− (ref. 50), dipeptide (Gly-Leu)51, histidine52 or JA-Ile33. NPF3-mediated transport of GA4 was not significantly affected by excess nitrate, dipeptide nor histidine and was weakly affected by JA-Ile. In comparison, NPF4.1-mediated uptake of GA4 was weakly affected by excess histidine whereas JA-Ile strongly inhibited GA4 uptake (Fig. 4g, Supplementary Fig. 6c–d). These observations suggest that NPF3 is predominantly a GA transporter. In comparison, our and previous studies suggest that NPF4.1 is a multi-specific transporter capable of importing several structurally unrelated phytohormones including ABA, GA and JA-Ile.
Recent work has identified the GA-intermediate GA12 as a long-distance transported form of inactive GA in Arabidopsis20 and the GA-intermediate GA20 as a transported form in Pisum sativum53. Consequently, we tested whether NPF3 and NPF4.1 transported selected commercially available intermediates (GA9, GA12 and GA20) and the catabolite GA8 of the GA biosynthetic pathway. At pH5, GA9 and GA12 precursors of GA4 accumulated to very high levels in oocytes and to the same extent in NPF3- and NPF4.1-expressing and non-injected oocytes due to diffusion (Fig. 4h). We were therefore not able to determine whether NPF3 and NPF4.1 transport these two intermediates. In comparison, GA20 accumulated to detectable levels in oocytes expressing NPF3 and NPF4.1, but to barely detectable levels in non-injected oocytes (Fig. 4h). Similarly, GA8, catabolite of GA1, accumulated to detectable levels in oocytes expressing NPF3 and NPF4.1, but below detection levels in non-injected oocytes (Fig. 4h). This suggests that NPF3 is able to transport GA20 in Arabidopsis. Interestingly, transport of the GA8 catabolite by NPF3- and NPF4.1-expressing oocytes indicated that intercellular transport of GA catabolites may occur in Arabidopsis.
Phylogenetic analysis suggests that NPF3 is conserved in all plant lineages with orthologs sharing a high degree of identity26. We tested GA4 transport capability of the NPF3 orthologs in the grass Oryza sativa (OsNPF3.1) and the legume Medicago truncatula (MtNPF3.1)26. OsNPF3.1 and MtNPF3.1 imported GA4 into oocytes to similar levels as AtNPF3, which indicates functional conservation of GA transport activity in orthologous NPF3 transporters (Fig. 4i).
Finally, as several members of the NPF family have been shown to transport ABA and auxin12,30,33,34, we tested NPF3 transport activity towards these plant hormones at pH 5.5 and pH 7.5. NPF3 accumulated GA4 and ABA in oocytes to comparable levels (Supplementary Fig. 6f). Dual GA/ABA substrate specificity was also reported for NPF4.1, previously identified as an ABA transporter also permeable for GA3 (ref. 12). This suggests that ABA and GA transport may be linked through the dual specificity of several NPF transporters. Uptake of the auxin indole-3-acetic acid by NPF3 was similar to non-injected control oocytes (Supplementary Fig. 6e). Thus, it is possible that NPF3 in our experimental setup plays a particularly important role for GA-Fl uptake, but acts redundantly with at least, NPF4.1/AIT3 or other GA transporters with respect to transport of non-conjugated ABA and GA. Altogether, our results show that NPF3 is a GA transporter that is functionally conserved across dicot and monocots and that appears functionally redundant with additional GA transporters in the elongating root endodermis.
GAs are fundamental for many aspects of plant growth and development. Here we shed light on the cellular mechanisms regulating GA transport in the root by revealing that NPF3 is a GA importer. An important question that this study could not fully address is whether NPF3 regulates GA cellular influx to promote GA activity or to inhibit GA response by GA degradation and/or storage. However, the fact that the endodermis is known to have an important role in GA response54,55, and NPF3 overexpression results in hypersensitivity to high levels of GA suggests that NPF3 is functioning to promote GA response. Although this study reveals that NPF3 can transport GA in vitro, and GA-Fl in the root, the complete GA transport mechanism is not clear. Since cytosolic pH 7.5 is driving GA de-protonation through the ion trap mechanism, the majority of GA4 is expected to be captured, with the limited ability to move from cell to cell22. The presence of GA exporters might explain how GA moves locally at the tissue or cellular level; however, these are yet to be discovered. It is possible that putative GA efflux carriers act redundantly and are therefore difficult to identify in genetic screens.
The NPF family of proton-coupled transporters is involved in nitrogen assimilation in eukaryotes and bacteria. In most plant species, NPF members have evolved to transport nitrate as well as additional specialized metabolites and hormones. This complexity makes it difficult to assess the biological role of the NPF proteins. How a transporter recognizes such different metabolites and hormones is an intriguing question. An interesting example of such diversity is the dual-affinity-specificity nitrate/auxin transporter NRT1.1 (ref. 30). The dual sensor/transceptor model proposes that NO3− sensing function of NRT1.1 is due to its dual NO3−/auxin transport activity and that the NO3− signal transduced by NRT1.1 is an NO3−-dependent modification of auxin transport in lateral root development30. On top of the multisubstrate specificity, this and other recent studies suggest that several NPFs can transport GA33,34. These results present an additional level of regulation of the GA response. It is intriguing to consider how NPF3 transports two antagonistic hormones, GA and ABA (possibly with different affinities), while NPF3 is induced by ABA and repressed by GA. We hypothesize that differences in spatiotemporal expression pattern as well as differences in subcellular localization and transport affinity among the NPF transporters towards GAs might explain the complex specificity and redundancy of GA transport. We expect future studies to dissect the complex network of multisubstrate specificity versus functional redundancy towards the same substrate that have evolved in the NPF family.
Plant material and growth conditions
All Arabidopsis thaliana lines used in this work are in Col-0 background. T-DNA insertion mutants were obtained from the Arabidopsis Biological Resource Center and Nottingham Arabidopsis Stock Centre. Homozygous mutants were selected by PCR using primers listed in Supplementary Table 1.
Seeds were plated on medium containing 0.5 × Murashige-Skoog (MS) medium, 1% sucrose and 0.8% agar on vertical plates, stratified for 2 days at 4 °C then transferred to growth chambers (Percival CU41L5) at 21 °C, 100 μE m−2 S−1 light intensity under long day light (16 h light/8 h dark).
Cloning of NPF3 overexpression and reporter lines
NPF3 was amplified with primer combinations listed in Supplementary Table 2, cloned into pENTR/D-TOPO (Invitrogen K2400) and subsequently cloned into binary destination vectors using LR Gateway reaction (Invitrogen 11791). We have examined the phenotype and YFP fluorescence for 13 independent NPF3-YFP lines (Supplementary Fig. 5f). The lines were partially silenced at the T3 generation. We continued with two lines that showed reduced silencing and high NPF3 RNA level (line #1 and 9; Supplementary Figs 1d and 5). All experiments were carried out with p35S:NPF3-YFP#9 unless otherwise indicated.
Hormone and inhibitor application
Chemicals were supplied to the agar medium at concentrations as indicated for each experiment in figure legends (starting from 10 mM stock solutions). Seedlings were placed on agar plates and roots were uniformly supplemented with chemicals. GA-Fl (5 μM) was applied in liquid MS media. Time points and chemicals concentrations are indicated for each experiment in the figure legend.
Imaging and analysis
Seedlings were stained in 10 mg l−1 propidium iodide (PI) for 1 min, rinsed and mounted in water. Seedlings were imaged on a laser scanning confocal microscope (Zeiss LSM 780 inverted microscope), with argon laser set at 488 nm for fluorescein excitation, 561 nm laser for PI excitation. Emission filters used were 493–548 nm filter for fluorescein derivatives, and 583–718 nm filter for PI emission. Image analysis and signal quantification were done with the measurement function of ZEN lite 2012 software. The number of quantified biological repeats and sampling points is indicated for each graph in figure legends.
Two-tailed Student’s t-test was performed whenever two groups were compared. Statistical significance was determined at P<0.001 unless otherwise indicated.
Luciferase reporter assay
Transgenic lines expressing luciferase under NPF3 promotor of 2Kb upstream of the ATG start codon, designated pNPF3:LUC, were grown for 10 days on MS horizontal plates and sprayed with solution containing 1 mM potassium luciferin (Promega E1601) and 2% Triton X-100. Plants were assayed for luciferase activity 14 h after spraying using BioSpace PhotonIMAGER. Plates were then flooded with liquid MS with or without 10 μM GA3 and assayed again at indicated times. Luminescence was quantified using M3Vision Software.
To assess germination, seeds were plated on horizontal MS plates, germination rate determined as seed coat rupture after 2 days scored under a Zeiss Stemi 2000-C stereo microscope.
For root and hypocotyl length measurements, seedlings were imaged using Zeiss Stemi 2000-C stereo microscope and measured using ImageJ software (http://rsbweb.nih.gov/ij/index.html).
To assess etiolation, seedlings of indicated lines were sown on sucrose free MS, exposed to 100 μE m−2 S−1 fluorescent light for 4 h, followed by 3 days at the dark. Hypocotyl length quantified as described above.
For root GA response assays, seeds were germinated on MS were transferred to 5 μM paclo after 4 days. On the next day, root length was marked. 1 μl of 5 μM GA3 diluted in water was applied to root tips for the three subsequent days. Roots were imaged and measured on day 10.
For all experiments except results presented in Fig. 2f and Supplementary Fig. 5c, total RNA was isolated from the indicated plant materials using RNeasy Plant Mini Kit (QIAGN 74,904). DNA was removed by RQ1 RNase-free DNase (Promega M6101). Total RNA (2 μg) converted to complementary DNA (cDNA) using M-MLV Reverse Transcriptase (Promega M1701) with oligo(dT)15 primer according to manufacturer protocols. Quantitative RT–PCR was performed with 40 ng cDNA in a final volume of 10 μl with Fast SYBR Green Master Mix (ABI 4385612) using Step One Plus System and software (ABI). The reaction conditions included 40 amplification cycles, (3 s at 95 °C; 30 s at 60 °C). Three technical repeats were performed for each cDNA sample, and at least three biological repeats were used for each treatment. The relative quantification was calculated with the ΔΔCt method, PP2A used as reference gene. Primers are specified in Supplementary Table 3. For results presented in Fig. 2f and Supplementary Fig. 5c, plant materials were transferred to 5 μM paclo following germination on MS plates. After 6 additional days, seedlings were treated with 10 μM GA4 in liquid MS for the indicated time periods. Total RNA was isolated from plants using NucleoSpin RNA plant kit and DNA was removed by an on-column treatment with rDNase (Macherey-Nagel, Düren, Germany). 2 μg of total RNA was subsequently reverse transcribed with M-MuLV Reverse Transcriptase (Fermentas, St Leon-Rot, Germany) using an oligo(dT) primer. The cDNA equivalent of 30–50 ng of total RNA was used in a 10 μl PCR reaction in a CFX96 Real-Time System Cycler (BioRad, Freiburg, Germany) with SsoAdvanced Universal SYBR Green Supermix (Bio-Rad, München, Germany) with three technical replicates in a CFX96 Real-Time System Cycler (Bio-Rad) in a 40-cycle step amplification protocol (10 s at 95 °C; 25 s at 60 °C). The relative quantification was calculated with the ΔΔCt method and ACT8 as a control. Relevant primers used are listed in Supplementary Table 3.
NPF3 trafficking analysis
p35S:NPF3-YFP seedlings were grown for 5 days on MS plates, transferred to 10 μM paclo or mock plates for 2 additional days, then treated with 10 μM GA4 or mock for 2 h in liquid media. Before imaging, seedlings were stained with 2 μM FM4-64 (mock) or FM4-64 with BFA for 15 min.
Gene synthesis and cloning for transport assays
The genes NPF3, NPF4.1, NPF2.10, NPF2.11 and NPF5.7 were part of a previously published transporter library56. Os06g15370 (OsNPF3.1) and Medtr5g055000 (MtNPF3.1) were synthesized by ThermoFisher Scientific Geneart with USER overhangs56,57. Coding sequences were cloned into the pNB1 oocyte expression vector58 that was made USER cloning compatible56,57 and verified by sequencing.
Oocyte preparation and complementary RNA injection
Xenopus oocytes were purchased as defolliculated Xenopus oocytes (stages V–VI) from Ecocyte Biosciences (Germany). Injection of 50 nl complementary RNA (500 ng μl−1) into Xenopus oocytes was done using a Drummond NANOJECT II (Drummond Scientific). Oocytes were incubated for 3 days at 17 °C in Kulori (90 mM NaCl, 1 mM KCl, 1 mM MgCl2, 10 mM MES) pH 7.5 before assaying.
Hormone uptake assays
GA3, indole-3-acetic acid, ABA, Gly-Leu, Histidine and GA4 were obtained from Sigma-Aldrich, GA1 was obtained from Toronto Research Chemicals, GA3-Fl and GA4-Fl were synthesized and characterized as previously described23. Briefly, N-Boc-2,2′-(ethylenedioxy) diethylamine was first reacted with 5-(and-6)-carboxyfluorescein succinimidyl ester to form a fluorescein-linker. Following deprotection, fluorescein-linker was conjugated to the C6 carboxylic acid of either GA3 or GA4 to form the corresponding GA3-Fl or GA4-Fl, respectively. GA12, GA20, GA9, GA8 and JA-Ile were obtained from OlChemIm Ltd. (Czech Republic). Xenopus uptake assays were carried out as follows: oocytes were preincubated in Kulori pH5 for 5 min, transferred to Kulori pH 5 with substrate for 60 min incubation, followed by four washes and transferred to Eppendorf tubes (one oocyte per tube or five oocytes). Excess washing buffer was removed and oocytes were busted in 50 μl of 50% MeOH and the homogenate was left in the freezer for 2 h. This was followed by centrifugation at 20,000g for 15 min to pellet remaining proteins. The supernatant was transferred to new tubes and diluted with 60 μl H2O. The diluted samples were then filtered through a 0.45 μm PVDF-based filter plate (MSHVN4550, Merck Millipore) and subsequently analysed by analytical LC-MS. Extracted data were analysed using Microsoft Excel, statistical analysis and data plotting were done using SigmaPlot version 13.0 (Systat software, USA).
Analysis of hormones and hormone-analogs by LC-MS
Compounds in extracts were directly analysed by LC-MS/MS. Chromatography was performed on an Advance UHPLC system (Bruker, Bremen, Germany). Separation was achieved on a Kinetex 1.7 u XB-C18 column (100 × 2.1 mm, 1.7 μm, 100 Å, Phenomenex, Torrance, CA, USA). Formic acid (0.05%) in water and acetonitrile (supplied with 0.05% formic acid) were employed as mobile phases A and B, respectively. The elution profile was: 0–0.2 min, 2% B; 0.2–0.9 min, 2–30% B; 0.9–3.2 min 30–100% B, 3.2–3.7 min 100%; 3.7.–3.8 min 100–2% B and 3.8–5.0 min 2% B. The mobile phase flow rate was 400 μl min−1. The column temperature was maintained at 40 °C. The liquid chromatography was coupled to an EVOQ Elite TripleQuad mass spectrometer (Bruker) equipped with an electrospray ion source operated in combined positive and negative ionization mode. The instrument parameters were optimized by infusion experiments with pure standards. The ion spray voltage was maintained at −4,000 V for GA and Sinigrin and +4,000 V GA-fluorescein analysis, respectively. Cone temperature was set to 300 °C and cone gas to 20 p.s.i. Heated probe temperature was set to 200 °C and probe gas flow to 50 p.s.i. Nebulizing gas was set to 60 p.s.i. and collision gas to 1.6 mTorr. Nitrogen was used as probe and nebulizing gas and argon as collision gas. Active exhaust was constantly on. Multiple reaction monitoring (MRM) was used to monitor analyte parent ion→product ion transitions: MRM transitions were chosen based on direct infusion experiments. Detailed values for mass transitions can be found in Supplementary Table 4. Both Q1 and Q3 quadrupoles were maintained at unit resolution. Bruker MS Workstation software (Version 8.2, Bruker) was used for data acquisition and processing. Linearity in ionization efficiencies were verified by analysing dilution series of standard mixtures. Sinigrin was used as internal standard but not used for quantification. Quantification of all compounds was achieved by external standard curves diluted with the same matrix as the actual samples. Identification of all analytes was achieved by their specific MRM transitions and by chromatographic separation (Supplementary Figs 7, 8 and Supplementary Table 4).
For data presented in Fig. 1b,c and Supplementary Fig. 1a chromatography was performed on an Agilent 1,100 Series LC (Agilent Technologies, Germany). Separation was achieved on a Zorbax SB-C18 column (Agilent; 1.8 μm, 2.1 × 50 mm) at a flow rate of 0.2 ml min−1. Formic acid (0.1%) in water and acetonitrile (supplied with 0.1% formic acid) were employed as mobile phases A and B, respectively. The elution profile was: 0–0.5 min, isocratic 6% B; 0.5–12.5 min, linear gradient 6–55% B; 12.5–13.1 min, linear gradient 55–95% B; 13.1–15.5 isocratic 95% B; 15.60–20 min, isocratic 6% B. The flow rate was increased to 0.3 ml min−1 in the interval 15.2–17.5 min. The column temperature was maintained at 35 °C. The Bruker HCT-Ultra ion trap mass spectrometer (Bruker Daltonics) was run in positive electrospray mode. Bruker MS Workstation software (Bruker) was used for data acquisition and processing. Linearity in ionization efficiencies were verified by analysing dilution series of standard mixtures. Quantification of all compounds was achieved by external standard curves diluted with the same matrix as the actual samples.
Predicted topology of NPF3
Topologies were defined by the online HMM-top tool (http://www.enzim.hu/hmmtop/) and visualized by the TMRPres2D software (http://biophysics.biol.uoa.gr/TMRPres2D/download.jsp).
Phylogenetic tree of the Arabidopsis NRT/PTR family
Protein sequences for Arabidopsis thaliana NRT/PTR family members were retrieved from TAIR (https://www.arabidopsis.org). Phylogenetic relationship was defined using (http://www.phylogeny.fr/)59,60,61,62 and visualized with FigTree software (http://tree.bio.ed.ac.uk/software/figtree/).
How to cite this article: Tal, I. et al. The Arabidopsis NPF3 protein is a GA transporter. Nat. Commun. 7:11486 doi: 10.1038/ncomms11486 (2016).
Durbak, A., Yao, H. & McSteen, P. Hormone signaling in plant development. Curr. Opin. Plant Biol. 15, 92–96 (2012).
Wolters, H. & Jurgens, G. Survival of the flexible: hormonal growth control and adaptation in plant development. Nat. Rev. Genet. 10, 305–317 (2009).
Oliva, M., Farcot, E. & Vernoux, T. Plant hormone signaling during development: insights from computational models. Curr. Opin. Plant Biol. 16, 19–24 (2013).
Boursiac, Y. et al. ABA transport and transporters. Trends Plant Sci. 18, 325–333 (2013).
Petrasek, J. & Friml, J. Auxin transport routes in plant development. Development 136, 2675–2688 (2009).
Kuromori, T. et al. ABC transporter AtABCG25 is involved in abscisic acid transport and responses. Proc. Natl Acad. Sci. USA 107, 2361–2366 (2010).
Kretzschmar, T. et al. A petunia ABC protein controls strigolactone-dependent symbiotic signalling and branching. Nature 483, 341–344 (2012).
Ko, D. et al. Arabidopsis ABCG14 is essential for the root-to-shoot translocation of cytokinin. Proc. Natl Acad. Sci. USA 111, 7150–7155 (2014).
Zhang, K. et al. Arabidopsis ABCG14 protein controls the acropetal translocation of root-synthesized cytokinins. Nat. Commun. 5, 3274 (2014).
Blilou, I. et al. The PIN auxin efflux facilitator network controls growth and patterning in Arabidopsis roots. Nature 433, 39–44 (2005).
Vanneste, S. & Friml, J. Auxin: a trigger for change in plant development. Cell 136, 1005–1016 (2009).
Kanno, Y. et al. Identification of an abscisic acid transporter by functional screening using the receptor complex as a sensor. Proc. Natl Acad. Sci. USA 109, 9653–9658 (2012).
Hedden, P. The genes of the Green Revolution. Trends Genet. 19, 5–9 (2003).
Ragni, L. et al. Mobile gibberellin directly stimulates Arabidopsis hypocotyl xylem expansion. Plant Cell 23, 1322–1336 (2011).
Eriksson, S., Bohlenius, H., Moritz, T. & Nilsson, O. GA4 is the active gibberellin in the regulation of LEAFY transcription and Arabidopsis floral initiation. Plant Cell 18, 2172–2181 (2006).
Dayan, J. et al. Leaf-induced gibberellin signaling is essential for internode elongation, cambial activity, and fiber differentiation in tobacco stems. Plant Cell 24, 66–79 (2012).
Phillips, I. & Hartung, W. Longitudinal and lateral transport of [3, 4‐3H‐] gibberelling A1 and 3‐Indoly (acetic acid‐2‐14C) in upright and geo-tropically responding green internode segments from helanthus annuus. New Phytol. 76, 1–9 (1976).
Altman, A. & Mozes, R. Comparative basipetal transport of 6-benzylaminopurine-8‐14C, gibberellin A3‐3H, IAA‐2‐14C, and sucrose‐14C in the root of intact citrus aurantium seedlings. Physiol. Plant. 39, 233–235 (1977).
Nash, L. J. & Crozier, A. Translocation and metabolism of [3H] gibberellins by light-grown Phaseolus coccineus seedlings. Planta 127, 221–231 (1975).
Regnault, T. et al. The gibberellin precursor GA12 acts as a long-distance growth signal in Arabidopsis. Nat. Plants 1, 15073 (2015).
Mander, L. N. The chemistry of gibberellins: an overview. Chem. Rev. 92, 573–612 (1992).
Kramer, E. M. How far can a molecule of weak acid travel in the apoplast or xylem? Plant Physiol. 141, 1233–1236 (2006).
Shani, E. et al. Gibberellins accumulate in the elongating endodermal cells of Arabidopsis root. Proc. Natl Acad. Sci. USA 110, 4834–4839 (2013).
Band, L. R. & Bennett, M. J. Mapping the site of action of the Green Revolution hormone gibberellin. Proc. Natl Acad. Sci. USA 110, 4443–4444 (2013).
Garcia, O., Bouige, P., Forestier, C. & Dassa, E. Inventory and comparative analysis of rice and Arabidopsis ATP-binding cassette (ABC) systems. J. Mol. Biol. 343, 249–265 (2004).
Leran, S. et al. A unified nomenclature of NITRATE TRANSPORTER 1/PEPTIDE TRANSPORTER family members in plants. Trends Plant Sci. 19, 5–9 (2014).
Kang, J. et al. PDR-type ABC transporter mediates cellular uptake of the phytohormone abscisic acid. Proc. Natl Acad. Sci. USA 107, 2355–2360 (2010).
Mravec, J. et al. Interaction of PIN and PGP transport mechanisms in auxin distribution-dependent development. Development 135, 3345–3354 (2008).
Geisler, M. & Murphy, A. S. The ABC of auxin transport: the role of p-glycoproteins in plant development. FEBS Lett. 580, 1094–1102 (2006).
Krouk, G. et al. Nitrate-regulated auxin transport by NRT1. 1 defines a mechanism for nutrient sensing in plants. Dev. Cell 18, 927–937 (2010).
Pike, S. et al. Members of the NPF3 transporter subfamily encode pathogen-inducible nitrate/nitrite transporters in grapevine and Arabidopsis. Plant Cell Physiol. 55, 162–170 (2014).
Sugiura, M., Georgescu, M. N. & Takahashi, M. A nitrite transporter associated with nitrite uptake by higher plant chloroplasts. Plant Cell Physiol. 48, 1022–1035 (2007).
Chiba, Y. et al. Identification of Arabidopsis thaliana NRT1/PTR family (NPF) proteins capable of transporting plant hormones. J. Plant Res. 128, 679–686 (2015).
Saito, H. et al. The jasmonate-responsive GTR1 transporter is required for gibberellin-mediated stamen development in Arabidopsis. Nat. Commun. 6, 6095 (2015).
Petrasek, J. et al. PIN proteins perform a rate-limiting function in cellular auxin efflux. Science 312, 914–918 (2006).
Friml, J. et al. Efflux-dependent auxin gradients establish the apical-basal axis of Arabidopsis. Nature 426, 147–153 (2003).
Barbez, E. et al. A novel putative auxin carrier family regulates intracellular auxin homeostasis in plants. Nature 485, 119–122 (2012).
Mravec, J. et al. Subcellular homeostasis of phytohormone auxin is mediated by the ER-localized PIN5 transporter. Nature 459, 1136–1140 (2009).
Ranocha, P. et al. Arabidopsis WAT1 is a vacuolar auxin transport facilitator required for auxin homoeostasis. Nat. Commun. 4, 2625 (2013).
Brady, S. M. et al. A high-resolution root spatiotemporal map reveals dominant expression patterns. Science 318, 801–806 (2007).
Mustroph, A. et al. Profiling translatomes of discrete cell populations resolves altered cellular priorities during hypoxia in Arabidopsis. Proc. Natl Acad. Sci. USA 106, 18843–18848 (2009).
Vieten, A. et al. Functional redundancy of PIN proteins is accompanied by auxin-dependent cross-regulation of PIN expression. Development 132, 4521–4531 (2005).
Goda, H. et al. The AtGenExpress hormone and chemical treatment data set: experimental design, data evaluation, model data analysis and data access. Plant J. 55, 526–542 (2008).
Böhmer, M. & Schroeder, J. I. Quantitative transcriptomic analysis of abscisic acid‐induced and reactive oxygen species‐dependent expression changes and proteomic profiling in Arabidopsis suspension cells. Plant J. 67, 105–118 (2011).
Kilian, J. et al. The AtGenExpress global stress expression data set: protocols, evaluation and model data analysis of UV‐B light, drought and cold stress responses. Plant J. 50, 347–363 (2007).
Sun, T., Goodman, H. M. & Ausubel, F. M. Cloning the Arabidopsis GA1 locus by genomic subtraction. Plant Cell 4, 119–128 (1992).
Regnault, T., Davière, J. M., Heintz, D., Lange, T. & Achard, P. The gibberellin biosynthetic genes AtKAO1 and AtKAO2 have overlapping roles throughout Arabidopsis development. Plant J. 80, 462–474 (2014).
Jorgensen, M. E. et al. A functional EXXEK motif is essential for proton coupling and active glucosinolate transport by NPF2.11. Plant Cell Physiol. 56, 2340–2350 (2015).
Nour-Eldin, H. H. et al. NRT/PTR transporters are essential for translocation of glucosinolate defence compounds to seeds. Nature 488, 531–534 (2012).
Tsay, Y. F., Schroeder, J. I., Feldmann, K. A. & Crawford, N. M. The herbicide sensitivity gene CHL1 of Arabidopsis encodes a nitrate-inducible nitrate transporter. Cell 72, 705–713 (1993).
Chiang, C. S., Stacey, G. & Tsay, Y. F. Mechanisms and functional properties of two peptide transporters, AtPTR2 and fPTR2. J. Biol. Chem. 279, 30150–30157 (2004).
Frommer, W. B., Hummel, S. & Rentsch, D. Cloning of an Arabidopsis histidine transporting protein related to nitrate and peptide transporters. FEBS Lett. 347, 185–189 (1994).
Proebsting, W. M., Hedden, P., Lewis, M. J., Croker, S. J. & Proebsting, L. N. Gibberellin concentration and transport in genetic lines of pea: effects of grafting. Plant Physiol. 100, 1354–1360 (1992).
Ubeda-Tomas, S. et al. Root growth in Arabidopsis requires gibberellin/DELLA signalling in the endodermis. Nat. Cell Biol. 10, 625–628 (2008).
Ubeda-Tomas, S. et al. Gibberellin signaling in the endodermis controls Arabidopsis root meristem size. Curr. Biol. 19, 1194–1199 (2009).
Nour-Eldin, H. H., Nørholm, M. H. & Halkier, B. A. Screening for plant transporter function by expressing a normalized Arabidopsis full-length cDNA library in Xenopus oocytes. Plant Methods 2, 1 (2006).
Geu-Flores, F., Nour-Eldin, H. H., Nielsen, M. T. & Halkier, B. A. USER fusion: a rapid and efficient method for simultaneous fusion and cloning of multiple PCR products. Nucleic Acids Res. 35, e55 (2007).
MacAulay, N., Gether, U., Klærke, D. A. & Zeuthen, T. Water transport by the human Na+‐coupled glutamate cotransporter expressed in Xenopus oocytes. J. Physiol. 530, 367–378 (2001).
Dereeper, A., Audic, S., Claverie, J.-M. & Blanc, G. BLAST-EXPLORER helps you building datasets for phylogenetic analysis. BMC Evol. Biol. 10, 8 (2010).
Dereeper, A. et al. Phylogeny. fr: robust phylogenetic analysis for the non-specialist. Nucleic Acids Res. 36, W465–W469 (2008).
Guindon, S. & Gascuel, O. A simple, fast, and accurate algorithm to estimate large phylogenies by maximum likelihood. System. Biol. 52, 696–704 (2003).
Anisimova, M. & Gascuel, O. Approximate likelihood-ratio test for branches: a fast, accurate, and powerful alternative. System. Biol. 55, 539–552 (2006).
This work was supported by grants from the Israel Science Foundation (1832/14) and (2158/14; E.S.), the German Israeli Foundation for Scientific Research and Development (I-236-203.17-2014; C.S. and E.S.), Nirit and Michael Shaoul Fund for Visiting Scholars and Fellows (C.S. and E.S.), the Human Frontier Science Program (HFSP—RGY0075/2015; E.S. and H.H.N.-E.), the National Institutes of Health (GM43644; M.E.), the Howard Hughes Medical Institute (M.E.), the Gordon and Betty Moore Foundation (M.E.) and the Danish National Research Foundation (DNRF99).
The authors declare no competing financial interests.
About this article
Cite this article
Tal, I., Zhang, Y., Jørgensen, M. et al. The Arabidopsis NPF3 protein is a GA transporter. Nat Commun 7, 11486 (2016). https://doi.org/10.1038/ncomms11486
Plant Molecular Biology Reporter (2020)
New Phytologist (2020)
Exploring plant metabolic genomics: chemical diversity, metabolic complexity in the biosynthesis and transport of specialized metabolites with the tea plant as a model
Critical Reviews in Biotechnology (2020)
Enhanced coproduction of astaxanthin and lipids by the green microalga Chromochloris zofingiensis: Selected phytohormones as positive stimulators
Bioresource Technology (2020)
Signalling Overlaps between Nitrate and Auxin in Regulation of The Root System Architecture: Insights from the Arabidopsis thaliana
International Journal of Molecular Sciences (2020)