The ancient morphoregulatory hormone auxin dynamically realigns dedicated cellular processes that shape plant growth under prevailing environmental conditions. However, the nature of the stress-responsive signal altering auxin homeostasis remains elusive. Here we establish that the evolutionarily conserved plastidial retrograde signaling metabolite methylerythritol cyclodiphosphate (MEcPP) controls adaptive growth by dual transcriptional and post-translational regulatory inputs that modulate auxin levels and distribution patterns in response to stress. We demonstrate that in vivo accumulation or exogenous application of MEcPP alters the expression of two auxin reporters, DR5:GFP and DII-VENUS, and reduces the abundance of the auxin-efflux carrier PIN-FORMED1 (PIN1) at the plasma membrane. However, pharmacological intervention with clathrin-mediated endocytosis blocks the PIN1 reduction. This study provides insight into the interplay between these two indispensable signaling metabolites by establishing the mode of MEcPP action in altering auxin homeostasis, and as such, positioning plastidial function as the primary driver of adaptive growth.
Plant adaptive growth is a central strategy evolved through integration and coordination of a complex composite of signaling pathways to cope with inevitable environmental challenges. Auxin [indole-3-acetic acid (IAA)] is an indispensable hormone functional as a morphoregulatory informational output integrating developmental and environmental cues into a complex regulatory network enabling optimal architectural modifications both in plantae and eubacterial kingdoms1,2,3,4,5.
It is well established that sculpting and adjusting the duration of adaptive responses are in part regulated by the dynamic alterations in IAA levels and distribution patterns3,6,7,8,9,10. The flavin mono-oxygenases YUCCA (YUC) family of enzymes are the rate limiting step in IAA biosynthesis in plants11,12,13. The analyses of various yuc mutant combinations demonstrated the critical role of local auxin biosynthesis in seedling growth and developmental processes14,15. The dynamics of auxin response is often monitored using the synthetic auxin-responsive promoter DR5 or Aux/IAA auxin-interaction domain DII fused to a reporter, enabling the visualization of the spatial pattern of auxin response and thus auxin gradients16,17,18,19. The establishment of auxin gradients supported by cellular efflux requires the functional network of auxin-efflux carrier family of PIN-FORMED (PIN) proteins comprised of eight members in Arabidopsis20. The founding family member is PIN1, initially identified by characterization of the pin-formed1 mutant in Arabidopsis, is a recycling membrane protein localized on the basal side of cells in the vascular tissue21,22,23. The delivery of newly synthesized PIN1 to plasma membrane requires ARF guanine-nucleotide exchange factors (ARF-GEFs), BIG1 through BIG4, while the abundance of PIN1 at the plasma membrane, and the consequential auxin distribution is regulated by clathrin-mediated endocytosis23,24,25,26.
Beyond being a core regulator of an array of plant developmental processes including growth and architecture, auxin is also an instrumental hormone in tailoring responses to abiotic and biotic stimuli27. As such, the interplay between environmental inputs and the control on auxin levels and distribution patterns provide the plasticity required for plant’s survival, as reflected in stress-mediated morphogenic responses by reduced cell division and elongation28. In fact, auxin homeostasis refines plant responses to environmental signals by multiple mechanisms including modulation of reactive oxygen species (ROS) homeostasis, induction of ROS detoxification enzymes, and regulation of chloroplast protein import29,30,31,32. Reciprocally, auxin metabolism is regulated by plastidial enzymes such as the plastidial NADPH-thioredoxin reductase (NTRC). This enzyme is reported to be involved in regulation of auxin levels as evidenced by reduced auxin and hence retarded growth of ntrc mutant as compared to the control plants33. Collectively, these results have led to the assumption that plastidial stress-signaling metabolite(s) may play a role in maintaining auxin homeostasis and by extension regulation of plant adaptive responses. Specifically, a connection between auxin and plastid-to-nucleus (retrograde) signaling is suggested, and a role for auxin-based signaling as secondary components involved in the response cascades following a retrograde plastidial signal is assumed34.
The stunted growth phenotype of the ceh1 (constitutively expression HPL) mutant triggered our interest to explore the plausible connection between auxin and a stress-specific plastidial retrograde signaling metabolite in plant adaptive responses. Specifically, we questioned whether altered auxin homeostasis may contribute to the stunted phenotype of the ceh1 mutant, and if so how auxin homeostasis might be altered in this plant. The focus on ceh1 is because this mutant accumulates methylerythritol cyclodiphosphate (MEcPP), an essential bifunctional plastidial metabolite serving as a precursor of isoprenoids produced by the plastidial methylerythritol phosphate (MEP) pathway, as well as a stress-specific retrograde signal communicating environmental perturbations sensed by plastid-to-nucleus35,36,37,38,39. The MEP pathway is evolutionarily conserved, and MEcPP is produced not only by plantae but also by the non-photosynthetic “apicoplast” plastids of parasites such as the malarial parasite, and by eubacteria36,39. Intriguingly, stress-mediated accumulation of MEcPP in bacterial culture suggests the ancient nature and functional conservation of this metabolite beyond plantae36,39,40,41.
Here, using constitutive and inducible MEcPP accumulating lines, in concert with pharmacological interference with the flux through MEP pathway, and exogenous treatment of plants with MEcPP, enabled us to establish the specifc and the key role of this stress-specific plastidial retrograde signaling metabolite in modulating growth by reducing the abundance of auxin and its transporter PIN1 via dual transcriptional and post-translational regulatory inputs.
MEcPP-dependent reduction of IAA and PIN1 abundance
The stunted growth of the ceh1 prompted us to examine whether this compromised phenotype is caused by constitutively high MEcPP or by increased levels of salicylic acid (SA) in the mutant background39. These studies were further warranted by the established SA-mediated suppression of the auxin signaling42. Thus, we analyzed the hypocotyl length of seedlings in four genotypes P, ceh1, the SA deficient lines eds16, and ceh1 eds16 double mutant39. Similarly retarded growth of ceh1 and ceh1eds16 seedlings unequivocally demonstrate an SA-independent, but MEcPP-dependent inhibition of hypocotyl growth in ceh1 (Supplementary Fig. 1a–c).
Next, we examined the potential role of IAA in the stunted hypocotyl phenotype of ceh1 seedlings39. Measurements of IAA established the reduced levels of this growth hormone in ceh1 compared to lines originally employed in the genetic screen that identified ceh1, and thus designated as Parent (P) plants39 (Fig. 1a). Notable recovery of the ceh1 short hypocotyl phenotype by exogenous application of IAA reaffirmed the involvement of this growth hormone (Fig. 1b, c). Application of various concertation of auxin, however, did not result in an increased root length in ceh1. Nevertheless, low concentration of auxin (1 μM), resulted in a less severely reduced growth of roots in ceh1 compared to P plants (Supplementary Fig. 2). Collectively, these results suggest effectiveness of IAA in modulating both hypocotyl and root growth in ceh1 albeit at different degrees.
The established role of MEcPP as a key dynamic orchestrator of transcriptional network43 led us to question whether the reduced IAA level is in part due to alteration in transcript levels of YUCCA (YUC) genes encoding a family of enzymes catalyzing the rate limiting step in IAA biosynthesis11,12,13. The expression level analyses of YUC family members (YUC1 through YUC10) show reduced YUC3 and YUC5 transcripts in ceh1 compared to the P (Fig. 1d & Supplementary Fig. 3). This selectivity supports the earlier notion of an overlapping function among a subset of the YUCs15, and further promotes the tailored functionality of individual YUCs in response to specific stress signal(s).
Next, we monitored dynamics of auxin response using the synthetic auxin-responsive promoter DR5:GFP. The ceh1 mutant expressing DR5:GFP showed a ~70% reduction in DR5 expression as compared to P (Fig. 1e & Supplementary Fig. 4a).
To assess the contribution of auxin transport to the decreased DR5 promoter-driven GFP signal in the ceh1 mutant, we examined the transcript levels of the auxin-efflux carrier PIN-FORMED1 (PIN1), a recycling membrane protein localized on the basal side of cells in the vascular tissue23. Expression analyses of PIN1 in ceh1, followed by extended analyses in the four aforementioned genotypes demonstrated a reduction in PIN1 transcript levels exclusively in high MEcPP containing lines (Fig. 1f and Supplementary Fig. 4b). Furthermore, the combined approaches of Western blot and immunolocalization analyses confirmed a ~40% reduction in PIN1 protein levels in ceh1 compared with P (Fig. 1g-h & Supplementary Fig. 4c).
The physiological ramification of the altered auxin homeostasis in ceh1, especially in light of the reduced susceptibility of the mutant to auxin inhibition of root growth (Supplementary Fig. 2), led us to compare the root cell cycle in mutant versus the P plants. To examine the cell-cycle progression we employed EdU, a thymidine analog that incorporates only in DNA during replication, enabling a direct and quantitative measure at single-cell resolution at the root tips by the intrinsic root coordinate system (iRoCS) method44,45. The analyses of cell-cycle events in the root apical meristem (RAM) revealed reduced DNA replication and by extension cell division events in the ceh1 compared with the P (Supplementary Fig. 5a). Accordingly, the reduced cortex cell number in RAM resulted in shorter meristem size of ceh1 roots (Supplementary Fig. 5b).
To further examine the potential role of MEcPP in ceh1 mutant in reducing growth and altering auxin homeostasis as measured by the DR5:GFP signal, we employed a pharmacological approach using fosmidomycin (FSM), a MEP-pathway inhibitor (Fig. 2a). This inhibitor arrests the flux through the pathway and abolishes MEcPP-mediated formation of otherwise stress-induced subcellular structures known as ER bodies in the ceh1 mutant46,47. The analyses of DR5:GFP expression in 7-day-old seedlings grown in the presence of the inhibitor clearly show that while the FSM treatment did not modulate DR5 expression in P seedlings, it did recover the low DR5:GFP expression in ceh1/DR5:GFP seedlings to levels similar to that in P plants (Fig. 2b & Supplementary Fig. 6).
Collectively, these observations confirmed MEcPP-mediated alteration of auxin homeostasis as a key mechanism underpinning growth retardation in the ceh1 mutant.
Induction of MEcPP reduces the abundance of auxin and PIN1
To further explore the MEcPP potential function in altering auxin levels and PIN1 protein abundance, we generated dexamethasone (DEX) inducible RNAi lines of hydroxyl methyl butenyl diphosphate synthase (HDS), encoding the enzyme catalyzing the conversion of MEcPP to hydroxymethylbutenyl diphosphate39. Metabolic analyses showed increasing MEcPP levels at 48 and 72 h post DEX induction in concert with the reduction of auxin levels in HDS RNAi (HDSi) lines, as compared to P plants (Fig. 3a-b). In addition, Western blot analyses clearly illustrated decreasing PIN1 protein abundance in HDSi lines at 48 and 72 h post induction relative to levels examined in seedling analyzed immediately after induction (0 time) (Fig. 3c).
Collectively, the data from the inducible HDSi lines display a clear correlation between accumulation of MEcPP and a reduction in IAA and PIN1 abundance, thus further substantiate the finding obtained from constitutively producing MEcPP mutant plant (ceh1) and corroborate with FSM treatment results.
Exogenous MEcPP reduces auxin levels and PIN1 abundance
To test the functional specificity of MEcPP signaling in altering auxin homeostasis, we visualized auxin distribution in response to exogenous application of MEcPP in two well-established independent maker lines DR5:GFP and DII-VENUS16,17,18,19. We specifically examined the DR5:GFP signal in hypocotyls of Mock and MEcPP treated seedlings and established reduced GFP signal post MEcPP treatment (Fig. 4a & Supplementary Fig. 7a). As expected and in contrast, the DII-VENUS signal in roots of MEcPP treated seedlings was enhanced as compared to the mock treated seedlings (Fig. 4b). Collectively, these results illustrate MEcPP-mediated reduction of auxin concentration in hypocotyls and roots of plants exogenously treated with the metabolite.
Furthermore, we monitored PIN1 abundance in response to exogenously applied MEcPP by examining PIN1-immuno-signal intensity in hypocotyls in conjunction with PIN1-GFP signal in the roots. The analyses show a rapid reduction in PIN1-immuno-signal intensity and PIN1:GFP signal at 10 min post MEcPP treatment, followed by further reductions at the later time point (Fig. 4c-d). These results are in agreement with the reduced DR5:GFP and PIN1 abundance in the inducible HDSi lines, and constitutively high MEcPP containing ceh1 mutant plants (Supplementary Fig. 4a and 7a). The one inconsistency between these data set is the reduced expression of PIN1 in the ceh1 mutant as opposed to MEcPP-treated plants (Fig. 1f and Supplementary Fig. 7b). This suggests a MEcPP-mediated immediate and specific response at the PIN1 protein levels.
Next, we questioned whether the response to MEcPP action is specific to PIN1 or nonspecific extending to other plasma membrane proteins, such as PIN2 and PIN3, members of the PIN auxin-efflux carrier family and an unrelated plasma membrane marker, NPSN1248,49. Absence of any visible alteration in the signal intensity of PIN3 and NPSN12 proteins in hypocotyl following MEcPP application established specificity of PIN1 response (Supplementary Fig. 7c, d). Furthermore, the result led to the conclusion that the decrease in the PIN3 signal intensity in the ceh1 as compared to the P (Supplementary Fig. 7e) may be the consequence of general stress or due to the sustained decrease in auxin levels50. The modest reduction in PIN2:GFP signal in response to MEcPP application in roots however, suggest responsiveness of PIN2 to MEcPP albeit at a much lower magnitude than that of PIN1(Supplementary Fig. 8a). The YFP signal derived from the PIN unrelated plasma membrane protein NPSN12:YFP (Supplementary Fig. 8b) remains unaltered in responses to MEcPP treatment, thus further supporting targeted action of MEcPP.
High light alters IAA homeostasis
To assess the physiological relevance of MEcPP-mediated alteration of IAA homeostasis, we treated plants with high light (HL), a stress known to increase the MEcPP levels rapidly and transiently39. We specifically examined DR5:GFP distribution in conjunction with PIN1-immuno-signal intensity of P plants before and at various intervals of HL exposure (30, 60, and 90 min). These results demonstrate reduced DR5:GFP distribution and PIN1-immuno-density signal intensities at all the time points of HL treatment (Fig. 5a, b and Supplementary Fig. 9a). It is of note that the reduction in the PIN1-immuno-density signal is not supported by measurable changes in expression levels of PIN1 in response to increasing MEcPP levels by HL (Supplementary Fig. 9b-c). Concordance of the data with the aforementioned result (Supplementary Fig. 7b) and discordance with reduced expression of PIN1 in constitutively high MEcPP containing ceh1 (Fig. 1f), differentiates between the consequences of general stresses versus the MEcPP-specific responses, and further alludes to post-transcriptional regulatory action of MEcPP in reducing PIN1 abundance. The transient nature of the response is evident from the recovery of both DR5:GFP abundance and the PIN1-immuno-density signal coupled with the reduced MEcPP levels to the basal levels at 24 h post HL treatment (Fig. 5c, d and Supplementary Fig. 9d-f).
High light enhances clathrin-mediated endocytosis of PIN1
The specificity of MEcPP-mediated reduction of PIN1 abundance led to the question of whether the mode of MEcPP action is through internalization of PIN1 to the plasma membrane. Thus, we examined the potential role of BIG proteins required for delivery of newly synthesized and/or recycled PIN1 to the plasma membrane51. We specifically tested and compared PIN1-immuno-signal intensity in big2,3,4 and big1,2,4 mutant lines26 before and after HL treatment (Fig. 6a). The notable reduction of PIN1 signal intensity in both mutant lines in response to HL excludes BIG proteins as the MEcPP path of action.
Next, we exploited pharmacological interference with clathrin-dependent endocytosis of PIN1 using tyrosine analog tyrphostin A23 (TyrA23), a well-established inhibitor of recruitment of endocytic cargo into the clathrin-mediated pathway, together with tyrphostin A51 (TyrA51) a close structural analog of TyrA23 routinely used as a negative control25,52. The unaltered PIN1-immuno-density signal in HL/TyrA23 treated as opposed to those of HL and HL/TyrA51 treated plants is a clear demonstration of clathrin-dependent endocytosis route of action (Fig. 6b). This strongly supports the notion that MEcPP-mediated signal(s) enable a precise control of auxin fluxes through post-transcriptional regulation of PIN1 abundance at the plasma membrane.
Plants exquisitely tune and align their growth to prevailing environmental conditions. Underpinning this adaptation is auxin, the morphoregulatory hormone that dynamically realigns dedicated cellular processes that shape growth under standard and stress conditions. However, the nature of stress-responsive endogenous signaling molecule that regulates levels and distribution patterns of this hormone has remained elusive.
Here, the outcome of studies using constitutively and inducible MEcPP-producing lines in conjunction with pharmacological interference with the MEP pathway, and with exogenous application of MEcPP, established this stress-specific plastidial retrograde signal, MEcPP, as the upstream signal defining the optimal abundance of IAA and PIN1 via dual transcriptional and post-transcriptional regulatory inputs. Specifically, MEcPP accumulation in response to stress signals39,47 reduces growth by altering IAA level. Indeed, the pharmacological hinderance of flux though the MEP pathway substantiates the role of MEcPP in modulation of auxin abundance, as examined by DR5:GFP signal. Our data further support the notion that reduction in auxin levels is in part through decreased levels of YUC3 and 5 transcripts. It is of note that a previous report has clearly demonstrated that mutation in five YUC genes (YUC3, YUC5, YUC7, YUC8 and YUC9) resulted mainly in retarded development of roots, and not hypocotyls of mutant seedlings53. Accordingly, we propose that MEcPP-mediated stunted ceh1 hypocotyl growth is not exclusively due to reduced expression of YUC genes but it is also the result of reduced auxin transport.
The mode of MEcPP action in transcriptional suppression of YUC genes is yet to be determined, but the notion of integration of MEcPP into transcriptional networks and robust alteration of stress-response circuitry of selected genes is well established54,55,56,57. Indeed uncovering MEcPP mode of action in transcriptional regulation of auxin biosynthetic genes is central for gaining insight into the molecular basis of the interplay between these two ancient and essential signaling pathways.
Moreover, we demonstrate decreased auxin flux through reduced abundance of PIN1 in constitutive and inducible MEcPP-producing lines as well as in plants exposed to HL, a physiologically relevant stress that result in accumulation of MEcPP. This finding confirms the notion of HL-mediated initiation of retrograde signal(s) that lead to acclimatory responses58, and further identifies MEcPP as the stress-specific retrograde signal that accumulates as the result of HL treatment, mediating the observed adaptive responses. The reduced PIN1 protein abundance in the absence of any detectable changes in the polarity of this transporter, strongly suggests that MEcPP path of action is in reduction of PIN1 protein abundance and not via a change in the direction of auxin transport. In addition, targeted pharmacological interference with clathrin-dependent endocytosis of PIN1 identified post-transcriptional mode of MEcPP-mediated action through regulation of PIN1 abundance at the plasma membrane.
In summary, our results provide insight into the dynamic nature of plastidial regulation of auxin homeostasis and offer molecular evidence for the dual regulatory action of the stress-specific retrograde signaling metabolite, MEcPP, in modulating auxin and PIN1 abundance levels by transcriptional and post-translational regulatory inputs. A simplified schematic model depicts the dual path of MEcPP action constituting plastidial operational mode of function in adjusting growth and reallocation of resources to adaptive responses (Supplementary Fig. 10).
This work provides a coherent picture of how the interplay between MEcPP and auxin homeostasis provides plants with the plasticity necessary to exert a refined control over the continuous environmental variables. In addition, and of particular importance is the concept of stress-induced plastidial retrograde metabolite based signaling responsible for regulation of growth, thereby shifting the paradigm of the role of the plastid in plant adaptive responsiveness from that of a secondary player to that of an essential primary component. Furthermore, the interconnection between auxin and MEcPP, two ancient and essential signaling metabolites, provides a fresh perspective on the evolution of adaptive mechanisms.
Plant growth and treatments
All experiments were conducted on seedlings grown in long day (LD; 16-h light/8-h dark cycles), at ~22 °C on 1/2 × MS media. The seedlings used were ceh1 and Parent (the ceh1 background prior to EMS mutagenesis)39, HDSi lines (see below), DR5:GFP lines that were kindly provided by Mark Estelle, (PIN2:PIN2-GFP, PIN3:PIN3-GFP, NPSN12-YFP49,59,60), and DII-VENUS19, BIG mutant lines26.
MEcPP treatment was performed as previously described with slight modifications. Specifically, 7-old seedlings were treated with MEcPP prepared in 1/2 MS to the final concentration of 100 μM. The mock experiments were conducted with 1/2 MS.
Tyrphostin A23 and tyrphostin A51 treatments were conducted on 7-day-old seedlings grown under LD condition. Seedlings were treated for 60 min with DMSO (control), or 100 μM tyrphostin A23 and 100 μM tyrphostin A51. The treated seedlings were subsequently exposed to HL (800 μmol m−2sec−1) for 90 min prior to immunolocalization studies.
Hypocotyl length measurement
7-day-old seedlings were scanned using the Epson scanner, and ImageJ (from http://rsb.info.nih.gov/ij/) was used to measure the hypocotyl length.
Quantification of gene expression
Real-time quantitative PCR and data normalization were performed as described43,61,62, using Quantprime. Each experiment was performed on three biological replicates each with three technical replicates, using the primer sequences shown in Supplementary Table 1.
High light treatment
Plate grown 7-day old seedlings were exposed to HL (800 μmol m−2s−1) for 30 min, 60 min and 90 min, at a controlled temperature maintained at 22 °C. At each of the indicated time points, seedlings were collected for MEcPP measurement, RT-qPCR, immunolocalization and confocal imagining.
Immunolocalization of PIN1
The immunolocalization analyses were carried out according to the described method63 with some modifications. Specifically, we used 7-day-old seedlings that were fixed in 4% paraformaldehyde (PFA in MTSB) for 1 h at room temperature (RT). Upon removal of fixative the seedlings were initially washed with MTSB buffer and finally rinsed with H2O. Seedlings were them placed on adhesive coated slides till dry before covering them with a coverslip chamber and subsequent addition of 200 µl 2% Driselase Basidiomycetes sp (Sigma), followed by application of vacuum for 3 min, and 30 min incubation at RT for 30 min. Next seedlings were washed 5 times with 200 µl MTSB followed by addition of 200 µl of 10% DMSO + 3% Igepal (Sigma) and incubation at RT for 1 h. Seedlings were then thoroughly washed several times with 200 µl MTSB, followed by addition of 200 µl 5% BSA (Sigma) and application of vacuum, and subsequent incubation at RT for 1 h. Next 200 µl of PIN1 antibody (1:50) in 5% BSA was added to the chamber, followed by incubation at 4 °C overnight, and subsequent incubation at 37 °C for 2 h. The seedlings were then washed with 200 µl MTSB before application of 200 µl of FITC anti-mouse (1:400) secondary antibody (KPL, 02-18-06) in 5% BSA, and incubation at 37 °C for 2 h. Seedlings were subsequently rinsed several times with 200 µl MTSB. Next MTSB was removed and seedlings were incubated in equilibration buffer (Invitrogen Antifade Kit) for 10 min at RT. Lastly, antifade reagent (Invitrogen Antifade Kit) was added to the chamber and finally sealed the slides with nail polish for confocal imaging.
MEcPP and auxin measurements
MEcPP extraction and quantification were performed as previously described39,43. Briefly, samples were analyzed using a Dionex Ultimate 3000 binary RSLC system coupled to Thermo Q-Exactive Focus mass spectrometer with a heated electro spray ionization source. Plant samples and standards were separated using an Accucore-150-Amide-HILIC column (150 × 2.1 mm; particle size 2.6 µM; Thermo Scientific 16726-152130) with a guard column containing the same column matrix (Thermo Scientific 852-00; 16726-012105). The separation was conducted in isocratic conditions using 60% acetonitrile with 0.1% formic acid and 40% 50 mM ammonium formate buffer pH 4.5. Flow rate was kept at 150 µL/min and the volume injected was of 5 µL. The column was kept at room temperature. Mass spectra were acquired in negative ion mode under the following parameters: spray voltage, 4.5 KV; sheath gas flow rate of 15 and capillary temperature of 275 °C. Samples were quantified using an external standard curve of MEcPP (Echelon, I-M054) with concentrations of 200, 100, 75, 60, 45, 36, 27, 13.5, 6.75 µM and final quantification were normalized to starting fresh weight.
IAA extraction was performed as previously described by some modifications64,65. Specifically, plant materials were ground twice using bead beater (Mini-Beadbeater; Biospecs Products) under cryogenic condition, followed by extraction in isopropanol: water: HCl (2:1:2), and subsequent sonication and centrifugation for 5 min at 21,000 × g at 4 °C. Supernatants were collected and the pellets were re-extracted. Supernatants from both extractions were combined and filtered through a 0.22 μm PTFE filter (Waters, Milford, MA, USA). The samples were freeze dried (FreeZone Plus 4.5 Liter Cascade, LABCONCO, MO) and re-dissolved in of acetonitrile: water (80:20) and centrifuged (21,000 × g for 5 min) and transferred to liquid chromatography (LC) vials for injection.
Liquid chromatography and mass spectrometry
Samples were analyzed using a Dionex Ultimate 3000 binary RSLC system coupled to Thermo Q-Exactive Focus mass spectrometer with a heated electro spray ionization source. Samples separation and gradient elution was by acetonitrile containing 0.1 % formic acid (A) and water containing 0.1 % formic acid (B) by a gradient profile (t(min), %A, %B): (0, 5, 95), (20, 95, 5), (25, 95, 5), (25.01, 5, 95), (35, 5, 95), using a AcclaimTM RSLC 120 C18 column (100 × 2.1 mm, particle size 2.2 µM; Thermo Scientific 068982). The flow rate was maintained at 200 µl/min, and at 35 °C. Mass spectra in positive mode were acquired under the following conditions: spray voltage, 4.50 KV; sheath gas flow rate 45, auxiliary gas flow rate 20, sweep gas flow rate 2, capillary temperature of 250 °C, S-lens RF level 50 and auxiliary gas heater temperature 250 °C. For relative quantitation, peak area for each compound (MS2; Thermo Trace Finder Software) was normalized to weight.
Root zone analysis using iRoCS pipeline
Five days old seedlings of P and ceh1 were transferred to liquid ½ MS medium for 5 h. Thereafter 10 μm 5‐ethynyl‐2′‐deoxyuridine (EdU) was added for 90 min. Seedlings were fixed in 4% formaldehyde for 60 min in microtubule stabilization buffer45. EdU was detected according to the manufacturer’s manual with modifications previously described45. After EdU detection, roots were washed twice with distilled water for 10 min, incubated in 200 μg L−1 4′,6‐diamidino‐2‐phenylindole (DAPI) for 20 min, washed again with distilled water and mounted on slides with a 120 μm spacer using mounting medium (DAPI GOLD reagent; Thermo Fisher Scientific Inc., Waltham, MA, USA). DAPI/EdU‐stained samples were recorded using a confocal laser scanning microscope (ZEISS LSM 510 META NLO) with a LD LCI‐Plan‐Apochromat 25 × /0.8 DIC Imm Korr objective. For the DAPI excitation, a 740 nm Chameleon laser was used and emission was detected with a band pass filter (BP 390–465 IR); EdU excitation was at 488 nm and emission was detected with a band pass filter (BP 500–550 IR). Serial optical sections were reconstituted into 3D image stacks to a depth of 100 μm with in‐plane (x–y) voxel extents of 0.15 and 0.9 μm section spacing (z). Two or three overlapping images (tiles) were recorded for each root. Images were converted to hdf5 format and then stitched. Representative roots for each treatment were chosen for annotation. Nuclei, mitosis events and DNA replication events were annotated using the iRoCS Toolbox44. All analyses and graphical presentations were performed as described66.
Confocal fluorescence imaging was performed using a Leica TCS SP5 confocal microscope (Leica Microsystems) or a Zeiss LSM 880 upright (Zeiss international). The manufacturer’s default settings were used for imaging GFP-, VENUS-tagged proteins and FITC fluorophore. Fluorescence signal for DR5-GFP and DII-VENUS19 was detected with 10× water objective, PIN1-GFP, PIN1-FITC, PIN3-GFP, NPSN12-YFP, and PIN2:GFP59 were detected with 40× objective. Signal intensity quantifications were performed using the ImageJ software (imagej.nih.gov/ij/).
Western blot analyses
Protein extraction was performed on 7-day old P and ceh1 seedlings grown on a 1/2 × MS media. Tissue was frozen upon collection and grind in liquid nitrogen using protein extraction buffer (50 mM Tris-HCl, pH 8, 10 mM EDTA, 2 mM EGTA, 0.01% SDS, 1 mM DTT, 10 μM/ml Protease Inhibitor Cocktails (Sigma)). The extract was subsequently centrifuged at 10,000 RPM for 15 min at 4 °C. The supernatant was collected and protein concentration was measured using Thermo Scientific Pierce Micro BCA Assay according to manufacturer instructions. Protein concentration of samples were adjusted to 2 or 3 μg/μL in 5 × Laemmli Buffer, heated at 56 °C and subsequently separated on 10% SDS-PAGE gel and transferred onto nitrocellulose membranes. Blots were probed with anti-PIN1 monoclonal antibody (1:100)63 primary antibody and secondary anti-mouse- Horseradish peroxidase (HRP) (KPL, catalog no. 074-1806) (1:3000) and chemiluminescent reaction was performed using and Pierce ECL Western Blotting Substrate. Working solutions of the substrates were prepared according to the manufacturers’ instructions and added to the membranes. The membranes were placed in plastic sheet protectors. Each membrane was exposed to X-ray films and developed. The uncropped scans of the blots are shown in Supplementary Figs. 1d and 6b. The anti-PIN1 monoclonal antibody was produced in Klaus Palme’s laboratory.
Inducible RNAi line of HDS
Homozygous Dexamethasone (DEX) inducible HDSi lines were generated by transforming plants with RNAi pOpOff vector construct67 harboring the HDS cloned with primer sequences shown in Supplementary Table 1. The seedlings were grown under LD condition for 7 days before treatment with 30 µM of DEX, followed by sample collection at 0, 48, and 72 h post induction.
All of the experiments were performed with at least three biological replicates each with three technical replicates. Data are mean ± standard deviation (SD). These analyses were carried out via a two-tailed Student’s t tests or R program with a significance of P < 0.05.
The authors declare that all data supporting the findings of this study are available within the manuscript and its supplementary files.
Cheong, Y. H. et al. Transcriptional profiling reveals novel interactions between wounding, pathogen, abiotic stress, and hormonal responses in Arabidopsis. Plant Phys. 129, 661–677 (2002).
Gil, P. et al. BIG: a calossin-like protein required for polar auxin transport in Arabidopsis. Genes Dev. 15, 1985–1997 (2001).
Kazan, K. & Manners, J. M. Linking development to defense: auxin in plant-pathogen interactions. Trends Plant. Sci. 14, 373–382 (2009).
Navarro, L. et al. A plant miRNA contributes to antibacterial resistance by repressing auxin signaling. Science 312, 436–439 (2006).
Spaepen, S., Vanderleyden, J. & Remans, R. Indole-3-acetic acid in microbial and microorganism-plant signaling. FEMS Microbiol. Rev. 31, 425–448 (2007).
Iglesias, M. J., Terrile, M. C., Bartoli, C. G., D’Ippolito, S. & Casalongue, C. A. Auxin signaling participates in the adaptative response against oxidative stress and salinity by interacting with redox metabolism in Arabidopsis. Plant Mol. Biol. 74, 215–222 (2010).
Park, J. E. et al. GH3-mediated auxin homeostasis links growth regulation with stress adaptation response in Arabidopsis. J. Biol. Chem. 282, 10036–10046 (2007).
Orozco-Cardenas, M. & Ryan, C. A. Hydrogen peroxide is generated systemically in plant leaves by wounding and systemin via the octadecanoid pathway. Proc. Natl. Acad. Sci. USA 96, 6553–6557 (1999).
Rojo, E. et al. Reversible protein phosphorylation regulates jasmonic acid-dependent and -independent wound signal transduction pathways in Arabidopsis thaliana. Plant J. 13, 153–165 (1998).
Thornburg, R. W. & Li, X. Wounding Nicotiana tabacum leaves causes a decline in endogenous indole-3-acetic acid. Plant Physiol. 96, 802–805 (1991).
Dai, X. et al. The biochemical mechanism of auxin biosynthesis by an arabidopsis YUCCA flavin-containing monooxygenase. J. Biol. Chem. 288, 1448–57 (2013).
Nishimura, T. et al. Yucasin is a potent inhibitor of YUCCA, a key enzyme in auxin biosynthesis. Plant J. 77, 352–366 (2014).
Zhao, Y. et al. A role for flavin monooxygenase-like enzymes in auxin biosynthesis. Science 291, 306–309 (2001).
Cheng, Y., Dai, X. & Zhao, Y. Auxin biosynthesis by the YUCCA flavin monooxygenases controls the formation of floral organs and vascular tissues in Arabidopsis. Genes Dev. 20, 1790–1799 (2006).
Cheng, Y., Dai, X. & Zhao, Y. Auxin synthesized by the YUCCA flavin monooxygenases is essential for embryogenesis and leaf formation in Arabidopsis. Plant Cell 19, 2430–2439 (2007).
Friml, J. et al. AtPIN4 mediates sink-driven auxin gradients and root patterning in Arabidopsis. Cell 108, 661–673 (2002).
Sabatini, S. et al. An auxin-dependent distal organizer of pattern and polarity in the Arabidopsis root. Cell 99, 463–472 (1999).
Friml, J. et al. Efflux-dependent auxin gradients establish the apical-basal axis of Arabidopsis. Nature 426, 147–153 (2003).
Brunoud, G. et al. A novel sensor to map auxin response and distribution at high spatio-temporal resolution. Nature 482, 103–106 (2012).
Paponov, I. A., Teale, W. D., Trebar, M., Blilou, I. & Palme, K. The PIN auxin efflux facilitators: evolutionary and functional perspectives. Trends Plant. Sci. 10, 170–177 (2005).
Okada, K., Ueda, J., Komaki, M. K., Bell, C. J. & Shimura, Y. Requirement of the auxin polar transport system in early stages of arabidopsis floral bud formation. Plant Cell 3, 677–684 (1991).
Galweiler, L. et al. Regulation of polar auxin transport by AtPIN1 in Arabidopsis vascular tissue. Science 282, 2226–2230 (1998).
Geldner, N., Friml, J., Stierhof, Y. D., Jurgens, G. & Palme, K. Auxin transport inhibitors block PIN1 cycling and vesicle trafficking. Nature 413, 425–428 (2001).
Adamowski, M. & Friml, J. PIN-dependent auxin transport: action, regulation, and evolution. Plant Cell 27, 20–32 (2015).
Dhonukshe, P. et al. Clathrin-mediated constitutive endocytosis of PIN auxin efflux carriers in Arabidopsis. Curr. Biol. 17, 520–527 (2007).
Richter, S. et al. Delivery of endocytosed proteins to the cell-division plane requires change of pathway from recycling to secretion. eLife 3, e02131 (2014).
Robert, H. S. & Friml, J. Auxin and other signals on the move in plants. Nat. Chem. Biol. 5, 325–332 (2009).
Potters, G., Pasternak, T. P., Guisez, Y. & Jansen, M. A. Different stresses, similar morphogenic responses: integrating a plethora of pathways. Plant Cell Environ. 32, 158–169 (2009).
Zhong, R., Thompson, J., Ottesen, E. & Lamppa, G. K. A forward genetic screen to explore chloroplast protein import in vivo identifies Moco sulfurase, pivotal for ABA and IAA biosynthesis and purine turnover. Plant J. 63, 44–59 (2010).
Laskowski, M. J. et al. FQR1, a novel primary auxin-response gene, encodes a flavin mononucleotide-binding quinone reductase. Plant Physiol. 128, 578–590 (2002).
Tognetti, V. B., Muhlenbock, P. & Van Breusegem, F. Stress homeostasis - the redox and auxin perspective. Plant Cell Environ. 35, 321–333 (2012).
Yu, X. et al. Plastid-localized glutathione reductase2-regulated glutathione redox status is essential for Arabidopsis root apical meristem maintenance. Plant Cell 25, 4451–4468 (2013).
Lepisto, A. et al. Chloroplast NADPH-thioredoxin reductase interacts with photoperiodic development in Arabidopsis. Plant Phys. 149, 1261–1276 (2009).
Glasser, C. et al. Meta-analysis of retrograde signaling in Arabidopsis thaliana reveals a core module of genes embedded in complex cellular signaling networks. Mol. Plant 7, 1167–1190 (2014).
Bjornson, M. et al. Integrated omics analyses of retrograde signaling mutant delineate interrelated stress-response strata. Plant J. 91, 70–84 (2017).
de Souza, A., Wang, J. Z. & Dehesh, K. Retrograde signals: integrators of interorganellar communication and orchestrators of plant development. Annu. Rev. Plant. Biol. 68, 85–108 (2017).
Lemos, M. et al. The plastidial retrograde signal methyl erythritol cyclopyrophosphate is a regulator of salicylic acid and jasmonic acid crosstalk. J. Exp. Bot. 67, 1557–1566 (2016).
Wang, C. & Dehesh, K. From retrograde signaling to flowering time. Plant Signal. Behav. 10, e1022012 (2015).
Xiao, Y. et al. Retrograde signaling by the plastidial metabolite MEcPP regulates expression of nuclear stress-response genes. Cell 149, 1525–1535 (2012).
Ostrovsky, D. et al. Effect of oxidative stress on the biosynthesis of 2-C-methyl-D-erythritol-2,4-cyclopyrophosphate and isoprenoids by several bacterial strains. Arch. Microbiol. 171, 69–72 (1998).
Ostrovsky, D. et al. Synthesis of a new organic pyrophosphate in large quantities is induced in some bacteria by oxidative stress. Biofactors 3, 261–264 (1992).
Iglesias, M. J., Terrile, M. C. & Casalongue, C. A. Auxin and salicylic acid signalings counteract the regulation of adaptive responses to stress. Plant Signal. Behav. 6, 452–454 (2011).
Benn, G. et al. Plastidial metabolite MEcPP induces a transcriptionally centered stress-response hub via the transcription factor CAMTA3. Proc. Natl. Acad. Sci. USA 113, 8855–8860 (2016).
Schmidt, T. et al. The iRoCS Toolbox--3D analysis of the plant root apical meristem at cellular resolution. Plant J. 77, 806–814 (2014).
Pasternak, T. et al. Protocol: an improved and universal procedure for whole-mount immunolocalization in plants. Plant Methods 11, 50 (2015).
Gonzalez-Cabanelas, D. et al. The diversion of 2-C-methyl-D-erythritol-2,4-cyclodiphosphate from the 2-C-methyl-D-erythritol 4-phosphate pathway to hemiterpene glycosides mediates stress responses in Arabidopsis thaliana. Plant J. 82, 122–137 (2015).
Wang, J. Z. et al. Initiation of ER body formation and indole glucosinolate metabolism by the plastidial retrograde signaling metabolite, MEcPP. Mol. Plant 10, 1400–1416 (2017).
Alassimone, J., Naseer, S. & Geldner, N. A developmental framework for endodermal differentiation and polarity. Proc. Natl. Acad. Sci. USA 107, 5214–9 (2010).
Geldner, N. et al. Rapid, combinatorial analysis of membrane compartments in intact plants with a multicolor marker set. Plant J. 59, 169–178 (2009).
Baster, P. et al. SCF(TIR1/AFB)-auxin signalling regulates PIN vacuolar trafficking and auxin fluxes during root gravitropism. EMBO J. 32, 260–274 (2013).
Paciorek, T. et al. Auxin inhibits endocytosis and promotes its own efflux from cells. Nature 435, 1251–1256 (2005).
Banbury, D. N., Oakley, J. D., Sessions, R. B. & Banting, G. Tyrphostin A23 inhibits internalization of the transferrin receptor by perturbing the interaction between tyrosine motifs and the medium chain subunit of the AP-2 adaptor complex. J. Biol. Chem. 278, 12022–12028 (2003).
Chen, Q. et al. Auxin overproduction in shoots cannot rescue auxin deficiencies in Arabidopsis roots. Plant Cell Physiol. 55, 1072–1079 (2014).
Benn, G. et al. A key general stress response motif is regulated non-uniformly by CAMTA transcription factors. Plant J. 80, 82–92 (2014).
Wang, C. Q., Guthrie, C., Sarmast, M. K. & Dehesh, K. BBX19 interacts with CONSTANS to REPRESS FLOWERING LOCUS T transcription, defining a flowering time checkpoint in Arabidopsis. Plant Cell 26, 3589–3602 (2014).
Wang, C. Q., Sarmast, M. K., Jiang, J. & Dehesh, K. The transcriptional regulator BBX19 promotes hypocotyl growth by facilitating COP1-Mediated EARLY FLOWERING3 degradation in Arabidopsis. Plant Cell 27, 1128–1139 (2015).
Wang, J. Z. et al. Initiation of ER body formation and indole glucosinolate metabolism by the plastidial retrograde signaling metabolite, MEcPP. Mol. Plant 10, 1400–1416 (2017).
Gordon, M. J., Carmody, M., Albrecht, V. & Pogson, B. Systemic and local responses to repeated HL stress-induced retrograde signaling in Arabidopsis. Front. Plant Sci. 3, 303 (2013).
Xu, J. & Scheres, B. Dissection of Arabidopsis ADP-RIBOSYLATION FACTOR 1 function in epidermal cell polarity. Plant Cell 17, 525–536 (2005).
Zadnikova, P. et al. Role of PIN-mediated auxin efflux in apical hook development of Arabidopsis thaliana. Development 137, 607–617 (2010).
Walley, J. W. et al. Mechanical stress induces biotic and abiotic stress responses via a novel cis-element. PLoS Genet. 3, 1800–1812 (2007).
Czechowski, T., Stitt, M., Altmann, T., Udvardi, M. K. & Scheible, W. R. Genome-wide identification and testing of superior reference genes for transcript normalization in Arabidopsis. Plant Physiol. 139, 5–17 (2005).
Ditengou, F. A. et al. Mechanical induction of lateral root initiation in Arabidopsis thaliana. Proc. Natl. Acad. Sci. USA 105, 18818–18823 (2008).
Savchenko, T. et al. Arachidonic acid: an evolutionarily conserved signaling molecule modulates plant stress signaling networks. Plant Cell 22, 3193–3205 (2010).
Lemos, M. et al. The pastidial retrograde signal MEcPP is a regulator of SA and JA crosstalk. J. Exp. Bot. 67, 1557–66 (2016).
Pasternak, T. et al. A 3D digital atlas of the Nicotiana tabacum root tip and its use to investigate changes in the root apical meristem induced by the Agrobacterium 6b oncogene. Plant J. 92, 31–42 (2017).
Wielopolska, A., Townley, H., Moore, I., Waterhouse, P. & Helliwell, C. A high-throughput inducible RNAi vector for plants. Plant. Biotechnol. J. 3, 583–90 (2005).
The authors would like to thank Glenn Hicks for critical discussions. We also express our thanks to Drs. Jared Shaw and Edward Balmond for providing the chemically synthesized MEcPP. This work was supported by Bundesministerium für Bildung und Forschung (BMBF SYSBRA, SYSTEC, Microsystems), DLR and German Research Foundation (DFG SFB746, INST 39/839,840,841), and by the National Science Foundation (NSF) IOS-1036491, NSF IOS-1352478, and National Institutes of Health (NIH) R01GM107311 to K.D.
The authors declare no competing interests.
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