Leaf growth is a complex process that involves the action of diverse transcription factors (TFs) and their downstream gene regulatory networks. In this study, we focus on the functional characterization of the Arabidopsis thaliana TF GROWTH-REGULATING FACTOR9 (GRF9) and demonstrate that it exerts its negative effect on leaf growth by activating expression of the bZIP TF OBP3-RESPONSIVE GENE 3 (ORG3). While grf9 knockout mutants produce bigger incipient leaf primordia at the shoot apex, rosette leaves and petals than the wild type, the sizes of those organs are reduced in plants overexpressing GRF9 (GRF9ox). Cell measurements demonstrate that changes in leaf size result from alterations in cell numbers rather than cell sizes. Kinematic analysis and 5-ethynyl-2'-deoxyuridine (EdU) incorporation assay revealed that GRF9 restricts cell proliferation in the early developing leaf. Performing in vitro binding site selection, we identified the 6-base motif 5'-CTGACA-3' as the core binding site of GRF9. By global transcriptome profiling, electrophoretic mobility shift assay (EMSA) and chromatin immunoprecipitation (ChIP) we identified ORG3 as a direct downstream, and positively regulated target of GRF9. Genetic analysis of grf9 org3 and GRF9ox org3 double mutants reveals that both transcription factors act in a regulatory cascade to control the final leaf dimensions by restricting cell number in the developing leaf.
Leaves are central plant organs that determine photosynthetic efficiency and thereby biomass production, yet the molecular mechanisms driving and controlling their growth and development are still far from being completely understood. Leaf growth—like other biological processes in different organisms—is controlled by an extensive network of genes that encode proteins of diverse cellular functions. Proteins controlling the activity of genes, called transcription factors, are particularly important for staging developmental processes. Here, we report how GRF9, a member of the so-called Growth-Regulating Factor (GRF) family of transcriptions factors, controls growth of leaves in the widely-studied model plant Arabidopsis thaliana, commonly known as thale cress. We show that GRF9 negatively controls final leaf dimensions by restricting cell number in the leaf primordium, while the size of the leaf cells remains unaltered. Using molecular techniques, we discovered that GRF9 acts within a regulatory cascade with another transcription factor, called ORG3. Furthermore, we show that GRF9 and ORG3 negatively control the organ size of flower petals, demonstrating that both transcription factors have a more general role in regulating organ size. Our study is one of the first reports to demonstrate a negative role of GRF transcription factors for organ growth.
Citation: Omidbakhshfard MA, Fujikura U, Olas JJ, Xue G-P, Balazadeh S, Mueller-Roeber B (2018) GROWTH-REGULATING FACTOR 9 negatively regulates arabidopsis leaf growth by controlling ORG3 and restricting cell proliferation in leaf primordia. PLoS Genet 14(7): e1007484. https://doi.org/10.1371/journal.pgen.1007484
Editor: R. Scott Poethig, Univerisity of Pennsylvania, UNITED STATES
Received: October 29, 2017; Accepted: June 13, 2018; Published: July 9, 2018
Copyright: © 2018 Omidbakhshfard et al. This is an open access article distributed under the terms of the Creative Commons Attribution License, which permits unrestricted use, distribution, and reproduction in any medium, provided the original author and source are credited.
Data Availability: Expression data are available from the NCBI Gene Expression Omnibus (GEO) repository (accession number GSE98490). All other relevant data are within the paper and its Supporting Information files.
Funding: The authors received no specific funding for this work.
Competing interests: The authors have declared that no competing interests exist.
Leaves are central photosynthetic organs of terrestrial plants; they determine photosynthesis efficiency and biomass production . The development of leaves is complex and involves the action of many different regulatory proteins including transcription factors [2–4]. A three-phase model has been proposed by which the cells at the shoot apical meristem (SAM) develop into a mature leaf, involving the initiation of a primordium derived from leaf founder cells, primary morphogenesis (cell proliferation), and secondary morphogenesis (elemental expansion); all three phases ultimately affect leaf size [4–10]. In Arabidopsis thaliana, phase one starts by the initiation of leaf primordia from cells located within the peripheral zone of the SAM, a process that lasts 2–3 days [3,11]. The transition from a leaf primordium with about 100 cells to a leaf with several thousand cells occurs during primary morphogenesis whereby massive cell proliferation (cell growth and division) occurs. In Arabidopsis leaves, the cell proliferation phase typically lasts 7–9 days. The rate and duration of cell proliferation are two important parameters that strongly affect final leaf size and shape [3,11]. Eventually, cell proliferation ceases in a basipetal (leaf tip to base) manner and secondary morphogenesis starts. Once initiated, the transition between cell proliferation and elemental expansion occurs rather abruptly, within a few days; the zone were cell proliferation ceases and cell elongation starts demarcates the so-called cell cycle arrest front (AF) [11–14]. AF progression is another major controlling step in determining leaf morphogenesis and final leaf size [4,12,15–17]. Secondary morphogenesis represents the longest phase of leaf development; it continues until the leaf reaches its final size. In this phase cells only expand [3,5,14].
Leaf growth and development is controlled by an extensive network of genes encoding different types of regulatory proteins, including many transcription factors (TFs) and several microRNAs [3,4,6,9,14,17–20]. Among them, GROWTH-REGULATING FACTORs (GRFs) represent a plant-specific TF family which has nine members in Arabidopsis thaliana (GRF1 –GRF9; ). Most members of this TF family are expressed in growing tissues, including leaves [21–24]. Functional and molecular analyses have shown that several GRFs contribute to the regulation of cell proliferation in leaf primordia and to organ separation in the shoot apical meristem [16,17,21–28]. GRFs do so by forming protein complexes with GRF-interacting factors (GIFs), which are transcriptional co-activators that function in determining leaf sizes [17,22,29–34]. The function of GRFs is further controlled by microRNA396 (miR396) which targets a number of GRFs including GRF1, 2, 3, 4, 7, 8, and 9 to control their expression [16,24,35–38].
Additionally, GRFs have been reported to coordinate plant growth with stress responses [38,39], to affect root and flower development [27,37,38,40,41], and to control plant longevity [24,42]. Interestingly, in contrast to the known positive functions of GRFs in cell proliferation, a recent study in maize (Zea mays) showed that ZmGRF10 functions as a negative regulator of cell proliferation in leaves . The authors showed that overexpression of ZmGRF10 results in smaller leaves due to a fewer number of cells which may result from a dominant negative effect of this protein on leaf growth by assembling an inactive GRF-GIF complex [17,34].
The establishment of the cell cycle arrest front (AF) is a complex cellular process that is not understood in its details so far. A known regulator of the process is the TCP transcription factor CINCINNATA (CIN), which controls the progression of the mitotic arrest front in snapdragon . Furthermore, cycling cells were closer to the base of developing leaves in miR396b overexpressors (35S:miR396b) than in the wild type, suggesting that this microRNA contributes to controlling the position of the AF, possibly by inhibiting GRF transcripts . In accordance with this, miR396 expression shows a gradient along the leaf axis, with a higher expression at the distal leaf part than the base; during leaf growth, the area of high miR396 expression extends towards the leaf base thereby progressively inhibiting GRF expression in the more proximal organ parts .
The importance of GRFs for setting the AF is further substantiated by the finding that the expression and protein levels of all three GIFs (GIF1—GIF3) in Arabidopsis are well correlated with changes in the cell cycle arrest front [22,31,44]. In accordance with this, overexpression of GIF1 (also known as AN3, ANGUSTIFOLIA3) delays the progression of the AF towards the base of the leaf . Similarly, overexpression of miR396-resistant GRF1 in maize results in an increased basal division zone in leaves and an increase of leaf length .
A further known player involved in establishing the AF during leaf development in Arabidopsis is KLUH/CYP78A5 (KLU), which appears to be involved in the formation of a mobile growth factor (MGF) and generating a concentration gradient of MGF in leaves . The proposed mobile factor has not been identified so far, leaving open the question how KLU controls the setting of the AF.
Here, we report that GRF9 from Arabidopsis thaliana functions as a negative regulator of leaf growth by restricting cell number within the incipient leaf primordium and restraining cell proliferation in the developing leaf. We also found direct binding of GRF9 to the promoter of OBP3-RESPONSIVE GENE 3 (ORG3), which has previously been shown to play a role in the early stages of leaf development , establishing a previously unknown GRF9 –ORG3 regulatory cascade.
Transcriptional pattern of the GRF9 gene
As GRF9 is not represented on the Arabidopsis ATH1 microarray, information about its expression pattern is limited. We therefore fused the GRF9 promoter (~1.5-kb promoter upstream the translation initiation codon) to the β-GLUCURONIDASE (GUS) reporter gene and tested the transcriptional activity of GRF9 in transgenic Arabidopsis plants (hereafter, ProGRF9:GUS). We observed GRF9 promoter-driven reporter activity throughout the entire young developing leaf of 3- to 5-day-old seedlings, and in the vascular tissue of cotyledons (S1A and S1B Fig). A more detailed analysis of 7- to 9-day-old seedlings revealed that GRF9 transcriptional activity is mostly restricted to the basal part of the developing leaf in which cells are still actively dividing (S1C Fig). In 10- to 12-day-old ProGRF9:GUS seedlings, reporter activity decreases in the leaf blade and remains mostly limited to the vascular tissues (S1D Fig). Similarly, reporter activity in mature leaves is mostly restricted to vascular strands (S1E and S1F Fig). Moreover, GRF9 transcriptional activity is dominant in the expanding zone of the roots and low, if detectable, in root tips (S1G and S1H Fig). In addition to vegetative tissues, GRF9 promoter-driven reporter activity is evident in reproductive parts of the plants, i.e. flowers (mostly carpels) and the abscission zone of siliques (S1I to S1P Fig). We next used quantitative real-time polymerase chain reaction (qRT-PCR) to measure GRF9 expression in different tissues and observed expression in leaves, flowers and roots; notably, expression in young leaves was higher than in the other tissues tested (S2A Fig). Expression of GRF9 in young leaves indicates a likely role in cell proliferation as shown for other GRFs [22–24]. Similarly, an analysis of previously reported transcriptome data obtained using tiling microarrays for third leaves of Arabidopsis at days 8–14 revealed high expression of GRF9 at days 8 and 9 when cell proliferation is high, but a decline of expression at day 10 when cell elongation starts (Table S1 in ). Thus, GRF9 transcript level follows the transcriptional activity pattern we observe here for ProGRF9:GUS seedlings.
Phytohormones, in particular auxin and cytokinin, affect cell proliferation [46–50]. We therefore tested the effect of auxin (applied as 2,4-D) and cytokinin (applied as zeatin) on GRF9 expression by qRT-PCR in 14-day-old wild-type (WT) seedlings treated with different concentrations of these phytohormones, but GRF9 expression level was not significantly altered in the conditions tested (S2B Fig). We also tested the effect of the hormones using ProGRF9:GUS lines, but did not observe a major effect (S2C Fig). These results indicate that GRF9 function is likely to be independent of auxin and cytokinin pathways as previously also reported e.g. for GRF7 .
grf9 mutants and GRF9 overexpressors have altered leaf size due to changes in cell number
To identify the biological role of GRF9, we selected two independent homozygous T-DNA insertion lines (grf9-1; SALK_140746; grf9-2; SAIL_324_G07; Fig 1A and 1B; S3 Fig) and Pro35S:GRF9 over-expression (GRF9ox1 and GRF9ox2) plants for further analyses (Fig 1B). Considering the prominent expression of GRF9 in young leaves, we characterized the leaf phenotypes of the grf9 mutants and GRF9ox lines. The loss-of-function grf9-1 and grf9-2 mutants developed enlarged rosettes with larger leaves compared to WT (114% and 123%, respectively; Fig 1C, 1E and 1F; S4A to S4C Fig) and a significantly increased cell number (112% and 115%; Fig 1G) while cell sizes within leaves remained unchanged (104% and 105%; Fig 1D and 1H). In contrast, GRF9ox1 and GRF9ox2 plants developed smaller leaves (87% and 85% of WT, respectively) with a decreased cell number (87% and 88%, respectively), while cell sizes were not affected (108% and 102%, respectively; Fig 1C–1H). In both grf9 mutants and the two GRF9ox plants, the leaf aspect ratio, defined as the leaf length over the leaf width, was close to that of the WT (Fig 1I). Collectively, the negative effect of GRF9 on leaf growth was observed in different photoperiods, namely in long-day (Fig 1C and 1F) as well as in short-day and equal-day conditions (S4A to S4C Fig).
(A) Schematic representation of the GRF9 locus and the locations of the T-DNA insertions (black triangles) in the grf9-1 and grf9-2 knockout mutants. White rectangles represent untranslated regions (UTRs), black rectangles show protein-coding regions, and thick connecting lines indicate introns. (B) Expression level of GRF9 determined by qRT-PCR in grf9 knockout and GRF9ox plants, compared to WT, for which expression is set to 1. No GRF9 expression was detected in grf9 knockout mutants (n.d.). The results are shown as means of three replicates ± SD. (C) Rosette phenotype. (D) Palisade cells of first-pair leaves of 21-day-old plants observed from a paradermal view. (E) Scans of representative first-pair leaves of WT, grf9-2 and GRF9ox1 seedlings. (F) Leaf sizes of WT, grf9 mutants and GRF9ox lines (n > 8 leaves). (G) Total number of palisade cells in the subepidermal layer of mature first leaves (n > 8 leaves). (H) Sizes of palisade cells observed from a paradermal view (n > 240 cells from more than eight leaves). (I) Leaf aspect ratio (ratio of leaf length to leaf width) of WT, grf9 mutants and GRF9ox plants. Means ± SD. Plants were grown for 3 weeks under a 16 h light / 8 h dark fluorescent illumination cycle at 120 μmol m-2 s-1. Asterisks in panels B, F and G indicate significant difference (Student's t-test; p < 0.05) from WT. Bars = 10 mm (panel C), 50 μm (panel D), and 5 mm (panel E).
To determine whether GRF9 affects leaf size at early stages of development, we embedded shoot apices of 2-day-old seedlings in paraffin and after sectioning analysed the size of incipient leaf primordia emerging from the SAM. As shown in Fig 2A and 2B, leaf primordium size was significantly increased in the grf9-2 mutants, but trended to be reduced in GRF9ox2 seedlings, compared to wild type. However, cell sizes in leaf primordia did not differ significantly between the genotypes (Fig 2C), indicating that more cells than in the WT contribute to the bigger primordia in grf9 seedlings, while the opposite appears to happen in GRF9 overexpressors. Of note, the size of the SAM–represented by the number of cells in the L1 layer—did not differ between the different genotpyes (Fig 2D), indicating that cell proliferation was more active in the incipient leaf primordia of grf9-2 than WT plants, but lower in those of GRF9ox2 plants. This conclusion is supported by a considerably higher expression of the G1-S phase cell cycle marker gene HISTONE4 (H4) in the leaf primordia and the SAM of grf9-2 compared to WT, as revealed by RNA in situ hybridization (Fig 2E and 2F). In addition, we analyzed the transcripts of another cell cycle activity gene, CYCLIN B1;1 (CYCB1;1), by RNA in situ hybridization. Similar to H4, we found higher CYCB1;1 transcript levels in the SAM of grf-2 mutant plants than the wild-type (S5 Fig).
(A) Emergence of first leaf primordia in 2-day-old WT, grf9-2 and GRF9ox2 plants grown in long day (LD) conditions (16 h light/8 h dark) analysed by toluidine blue staining. (B) Area of first leaf primordia of WT, grf9-2 and GRF9ox2 plants (n > 4 primordia). (C) Size of cells in leaf primordia of WT, grf9-2 and GRF9ox2 plants (n > 7 cells from more than four primordia). (D) Number of cells in the layer 1 (L1) of the SAM (n = 3 plants). (E) RNA in situ hybridization using HISTONE4 (H4) as probe on longitudinal sections of the apical meristem with young leaf primordia of 2-day-old WT and grf9-2 plants. (F) Number of cells expressing HISTONE4 (H4) at the SAM (n = 3 meristems). Error bars represent ± SEM. Scale bars 100 μm (panels A and E).
We also characterized the petal phenotype of grf9 mutants and GRF9ox plants. Notably, petal size was significantly increased in both, the grf9-1 and grf9-2 mutants (125% and 117%, respectively; S6A and S6B Fig) while the size of the petal cells remained unaltered (95% and 103%, respectively; S6C Fig). On the contrary, GRF9ox1 plants exhibited smaller petals with normal cell sizes (S6A to S6C Fig). Taken together, these results suggest that GRF9 contributes to determining final organ size by limiting cell proliferation during plant development.
Cell proliferation kinetics in developing leaves of grf9 and GRF9ox plants
As GRF9 affects cell proliferation already in the incipient leaf primordium, we wanted to know whether it also affects cell numbers subsequently, when leaves develop further. To address this, we performed a kinematic analysis of cell proliferation in young developing leaves (Fig 3). Cell number was determined by counting the number of adaxial subepidermal cells along the length of the first pair of leaves . As shown in Fig 3A, cell number increased in seedlings of all genotypes until day 10 to 12 and then did not change further thereafter. Cell numbers were significantly higher throughout the entire observation period in the two grf9 knockout mutants compared to WT, in accordance with a significantly bigger incipient leaf primordium in grf9 (see Fig 2B). Cell numbers were not significantly different between GRF9ox and WT seedlings at days 3 and 4 after germination, but were significantly lower in the overexpressors than the WT from day 5 onwards. We calculated the rate with which cell number increased during leaf development. As shown in Fig 3B, between days 3 and 4, cell numbers increased more in grf9 knockout mutants than in WT, while there was no detectable difference between WT and GRF9ox lines. At later stages of leaf development (from day 5 to day 10), cell numbers increased less prominently in GRF9ox seedlings than WT.
(A) Number of cells along the basal-apical axis of the first set of developing leaves in WT, grf9 knockout and GRF9ox lines. The curves show fitting to the experimental data with a polynomial function. R2 values are > 0.99 in all cases. At days 3 and 4 after germination, cell numbers are significantly higher in the two grf9 mutants than in WT (Student's t-test; day 3, p ≤ 0.01; day 4, p ≤ 0.001). At days 5 to 14, cell numbers are significantly higher in the two grf9 mutants than in WT, and significantly lower in the two GRF9ox lines (Student's t-test; P values between p ≤ 0.05 and p ≤ 0.001). Data are means of 6–14 leaves for the different genotypes and time points ± SD. The full data are given in S4 Table). (B) Increment of the number of cells in the adaxial subepidermal layer along the basal-apical leaf axis. Left: increment (Δ cell number) between day 3 and day 4 (D4-D3); right: increment between day 5 and day 10 (D10-D5) in WT and GRF9 transgenic plants. See S4 Table for the full data. (C) Relative expression levels of cell cycle-related genes in the leaf primordia from 7-day-old and 14-day-old WT, grf9-2 and GRF9ox1 plants. Gene expression in the WT is set to 1. Data are means ± SD (n > 8 seedlings).
We next assessed the expression of cell cycle marker genes: CYCB1;1 (CYCLIN-B1;1, B-class cyclin gene) and CYCB1;2, CYCD3;2 (CYCLIN-D3;2, D-class cyclin gene), and ANT (AINTEGUMENTA) [22,52–54] in developing leaves of 7- and 14-day-old seedlings, by qRT-PCR. We observed that expression of CYCD3;2, which encodes a key regulator of integrating cell division in lateral organ development [52,53], was similar in grf9, GRF9ox and WT in both, 7-day-old and 14-day-old plants (Fig 3C). We observed the same for CYCB1;1, CYCB1;2, and ANT, which function in cell proliferation and organ growth throughout plant development, supporting the model that cell proliferation rate in the later stages of developing leaves was not overtly affected in grf9 and GRF9ox plants.
grf9 mutants have an enhanced cell proliferation within the developing leaf
It has been reported that some GRFs and their interaction partners, such as GIF1 and the transcription factor TCP4, as well as miR396, are involved in controlling the progression of the AF, the boundary separating the cell proliferation from the cell differentiation area in the developing leaves [15,16,22,33,42,43,55]. Considering that GRF9 affects the size of the incipient leaf primordium and that cell number was affected in young leaves we considered the possibility that the area occupied by proliferating cells in the developing organ was changed in grf9 mutants. To test this, we visualized the proliferating cells in young leaves. One of the most accurate ways of distinguishing actively dividing from non-dividing cells is to directly detect DNA synthesis [56,57]. We therefore used the 5-ethynyl-2'-deoxyuridine (EdU) incorporation assay, which allows visualising S phase cells in animal and plant cells [44,56,58–61]. As expected, EdU signal is higher in the basal parts of young leaves where massive cell proliferation occurs, and the signal fades towards the distal part of the leaf (Fig 4A).
The first true leaves of 5-day-old seedlings were analysed. (A) Example of an EdU-stained Arabidopsis leaf. Green signals indicate cells undergoing mitosis. (B) EdU signal distribution in leaves, and (C) relative occupancy of proliferating cells within the developing leaves in grf9-2, GRF9ox1 and WT plants. Data represent average signals from at least eight seedlings.
More than eight observations revealed that the number of cells having detectable EdU signal was considerably increased in grf9 plants compared to WT. In contrast, GRF9ox plants showed a slight although insignificant decrease in the number of cells compared to WT (Fig 4B). We also determined the relative occupancy of the cell proliferation area relative to the total area of the leaf primordia in grf9, GRF9ox and WT plants, but did not detect significant differences between them (Fig 4C).
GRF9 binding site identification
Several GRF transcription factors affect leaf growth by regulating cell proliferation [21–24,29,62]. However, little is known about the downstream targets of these TFs and their gene regulatory networks. Therefore, to identify potential targets of GRF9, we first determined its binding site by in vitro binding site selection assay using the CELD fusion protein method . We identified the 6-base motif 5'-CTGACA-3' as the core GRF9 binding site (Fig 5A). Mutational analysis revealed that altering individual nucleotides within the identified core binding site dramatically diminished GRF9 binding activity (S7 Fig).
(A) GRF9 DNA-binding sequences determined using in vitro binding site selection. All selected oligonucleotides contain a functional GRF9-binding site as verified in DNA-binding assays. The nucleotides in the core binding sequence are shown in red. The logo of the GRF9 binding sequence profile was generated using the MEME program (http://meme.sdsc.edu/meme/cgi-bin/meme.cgi). (B) GRF9 binds in vitro to the ORG3 fragment harboring the GRF9 binding site. A schematic view of the ORG3 promoter (around 1.5 kb upstream of the translation start site) containing the GRF9 binding sequence (BS) is shown at the bottom (BS; black box). Electrophoretic mobility shift assay (EMSA) using GRF9-CELD protein and a 40-bp sequence of the ORG3 promoter harboring the GRF9 BS. GRF9-CELD protein incubated with those oligonucleotides causes retardation ('Band shift'). Retardation disappeared in the presence of competitor (unlabeled probe at high concentration) whilst adding a molar excess of mutated probe did not block the interaction between GRF9 protein and the labelled probe, indicating specific binding of GRF9 to the CTGACA binding site. (C) Laser scanning confocal microscopy images showing nuclear localization of GRF9-GFP fusion protein in 3-week-old transgenic Arabidopsis plants expressing GFP-tagged GRF9 protein. (D) Expression level of GRF9 and ORG3 in Pro35S:GRF9-GFP and WT (Col-0) plants. Expression was determined by qRT-PCR and values represent the means of replicates from three biological replicates ± SD. (E) GRF9 binds in vivo to the ORG3 promoter. ChIP-qPCR results of 5-day-old Pro35S:GRF9-GFP Arabidopsis seedlings. Data represent average enrichment (fold change, FC) in three independent biological replicates ± SD. (F) GRF9 transactivates the ORG3 promoter in vivo. Relative luciferase activity detected in Arabidopsis mesophyll cell protoplasts. Data are means ± SD of three independent transformations, each representing five technical replicates. The asterisks indicate significant difference (Student's t-test; p < 0.05).
Genes affected by GRF9
We next identified genes affected by GRF9, employing transgenic Arabidopsis plants expressing GRF9 from an estradiol (EST)-inducible promoter (hereafter, GRF9-IOE plants). We induced GRF9 expression by EST treatment for 3 and 4 h (using 2-week-old GRF9-IOE seedlings) and 6 h (using detached mature leaves from 4-week-old soil grown GRF9-IOE plants) and performed transcriptome profiling using Affymetrix ATH1 microarrays. We compared all three transcriptome data sets with those of the controls (mock treated with 0.15% ethanol) and identified 89 genes upregulated and five genes downregulated after EST treatment in at least two of the three time points (by at least 2-fold) (S1 Table). Twenty-three upregulated genes (including GRF9 itself) harbour at least one GRF9 binding site within their 1.5-kb promoters (S1 Table), identifying them as potential downstream targets of GRF9. Enhanced expression of most of the 23 genes was confirmed by qRT-PCR in independent biological samples of EST-induced GRF9-IOE seedlings (different induction times) as well as in the overexpression line GRF9ox1, while their expression was reduced in the grf9-1 knockout mutant (S8 Fig). Of note, expression of other AtGRFs and miR396 was not significantly altered after EST induction of GRF9 in the GRF9-IOE line, or in different GRF9 transgenic plants, respectively (S1 Table).
Based on their expression levels, harbouring of GRF9 binding site and literature review we selected OBP3-RESPONSIVE GENE 3 (ORG3), also known as bHLH039, as a potential target gene of GRF9 for further analysis.
GRF9 binds the ORG3 promoter in vitro
Regulation of gene expression involves the direct interaction of transcription factors with cis-regulatory elements located in the promoters of target genes. To investigate the physical interaction of GRF9 with the ORG3 promoter, we performed electrophoretic mobility shift assays (EMSAs). Sequence analysis of the ORG3 promoter (1.5 kb upstream of the translation start site) revealed the presence of one full-length GRF9 binding site (5'-CTGACA-3'; called BS in the following) ~1.3 upstream of its translation start site (Fig 5B). We tested interaction of recombinant GRF9 protein with a 40-bp long, 5'-DY682-labeled double-stranded oligonucleotide harbouring BS. As shown in Fig 5B, the DNA-protein complex migrated more slowly than free DNA indicating direct interaction of GRF9 with the labelled DNA. When unlabelled competitor DNA (oligonucleotide containing binding site) was added in molar excess, a strong reduction in signal intensity was observed; moreover, molar excess of the mutated version of the BS did not diminish binding to the correct BS (Fig 5B), confirming specificity of the interaction.
In vivo binding of GRF9 to the ORG3 promoter
To test whether GRF9 interacts in vivo with the ORG3 promoter, we performed chromatin immunoprecipitation (ChIP) and tested the enrichment of ORG3 promoter fragments by quantitative PCR (ChIP-qPCR), using transgenic Arabidopsis lines expressing GRF9-GFP fusion protein from the CaMV 35S promoter. As shown in Fig 5C, GRF9-GFP fusion protein accumulated in the nuclei of transgenic plants, consistent with its role as a transcription factor. In addition, ORG3 expression was elevated compared to WT in Pro35S:GRF9-GFP lines (Fig 5D), indicating that the GRF9-GFP fusion protein activated ORG3 similar to GRF9. Using these plants, we observed a significant enrichment of the ORG3 promoter region harbouring the GRF9 binding site (Fig 5E), supporting the conclusion that it is a direct downstream target of GRF9.
Transactivation of the ORG3 promoter in mesophyll cell protoplasts
To test whether ORG3 is transactivated by GRF9, we performed luciferase-based transactivation assays using Arabidopsis mesophyll cell protoplasts (Fig 5F). A reporter construct containing the firefly luciferase (FLuc) coding region under the control of the ~1.5-kb ORG3 promoter (ProORG3:FLuc) (Fig 5F) was transformed into protoplasts in the presence or absence of Pro35S:GRF9 effector plasmid. A significantly higher luciferase activity was observed when ProORG3:FLuc was co-transformed with Pro35S:GRF9 than in controls that were only transformed with the ProORG3:FLuc construct, indicating that GRF9 transactivates ORG3 expression in mesophyll cell protoplasts (Fig 5F). In the absence of Pro35S:GRF9, only low basal luciferase activity was observed (Fig 5F).
ORG3 restricts organ size
Our above results demonstrate that GRF9 positively regulates ORG3 expression by binding to its promoter, suggesting that GRF9 affects the cell proliferation process in developing leaves through ORG3. To address this point further, we characterized the impact of ORG3 on leaf development. First, we determined expression of ORG3 in two org3 knockout mutants (org3-1 and org3-2), both harbouring T-DNA insertions in the first exon (S9A and S9B Fig). Endpoint PCR as well as qRT-PCR revealed that accumulation of ORG3 transcripts in each line was drastically reduced in young seedlings of the two org3 mutant plants compared to WT (S9C and S9D Fig). Interestingly, both, org3-1 and org3-2 showed bigger leaves than WT (131% and 122%, respectively) with a significant increase in cell number (143% and 124%, respectively; Fig 6A–6C), like the two grf9 mutants (Fig 1E–1G). In contrast, the size of leaf cells was not affected in org3-1 and org3-2 mutants (Fig 6D). Our data therefore suggest that in leaves the loss of ORG3 causes a specific defect in cell proliferation. The same phenotype was found in petals in which loss of ORG3 caused increased petal size (S10A and S10B Fig). Cell size measurements showed that the size of the petal cells was not altered in org3-1 compared to WT (S10C Fig), indicating that the larger petals in org3 mutant are due to an increase in cell number. To estimate the impact of ORG3 on plant development, we produced overexpression lines of ORG3 (hereafter, ORG3ox1 and ORG3ox2) (S9D Fig). As a consequence, ORG3ox1 and ORG3ox2 plants showed significantly smaller leaves (75% and 68%, respectively) than the WT with a specific defect in cell proliferation (Fig 6). These results suggest that ORG3 restricts organ size by limiting cell number.
(A) Scans of representative first-pair leaves, (B) leaf size, (C) number of palisade cells, and (D) size of palisade cells (n > 240 cells) in WT, org3-1, org3-2, ORG3ox1 and ORG3ox2 plants. Results are expressed as percentage of WT ± SD. First-pair leaves from 21-day-old plants were analyzed (n > 8 in all cases). Asterisks indicate significant difference from WT (Student's t-test; p < 0.05). In (A), bar = 10 mm.
ORG3 acts downstream of GRF9
The molecular data reported in the previous sections, as well as the similar growth phenotypes observed in GRF9 and ORG3 overexpressors (reduced leaf sizes), and in grf9 and org3 knockout mutants (increased leaf sizes) suggested that GRF9 and ORG3 form a regulatory cascade in leaf development. To further substantiate this model, we created grf9-2 org3-1 and GRF9ox1 org3-1 double mutants (Fig 7, S9E and S9F Fig). We reasoned that simultaneously knocking out both genes would further increase leaf size (over the sizes of the single-gene mutants) if both transcription factors acted in independent biological pathways. However, as shown in Fig 7A–7D, leaf sizes, cell numbers and cell sizes of the grf9-2 org3-1 double mutant were not significantly different from those of the parent single-gene mutants, suggesting that ORG3 acts in the same pathway as GRF9 to regulate leaf development. Notably, while overexpression of GRF9 in the wild-type Col-0 background (GRF9ox plants) leads to reduced leaf size and cell number (Fig 1F and 1G; Fig 7A–7C), this effect is entirely lost when GRF9 is overexpressed in the org3-1 knockout mutant (Fig 7A–7C). Taken together, our data confirm a genetic interaction between GRF9 and ORG3, whereby ORG3 acts downstream of GRF9 to determine leaf size.
(A) Scans of representative first-pair leaves, (B) leaf area, (C) number of palisade cells, and (D) cell area of palisade cells (n > 240 cells) in WT, grf9-2, org3-1, org3-1 grf9-2 (line 7), GRF9ox1, and GRF9ox1 org3-1 (line 34) mutants. Data are expressed as a percentage of WT ± SD. First leaves from 21-day-old plants were analyzed (n > 8 in all cases). Asterisks in panels (B) and (C) indicate significant difference (Student's t-test; p < 0.05). In (A), bar = 10 mm.
Final leaf size has a major effect on photosynthetic performance and the formation of biomass . Leaf growth and development are controlled by a complex network of genes in which TFs are important controllers. In this study, we addressed the function of the transcription factor GRF9 for leaf growth in Arabidopsis. GRF9 belongs to the plant-specific GROWTH-REGULATING FACTOR (GRF) family, which in Arabidopsis includes nine members playing important biological roles [21–24,38,40,41,51,64,65].
Using ProGRF9:GUS reporter lines, we observed GRF9 reporter activity e.g. in the proliferation zone of developing leaves, similar to other members of the GRF family [22–24,34,66]. The transcriptional activity conferred by the GRF9 promoter broadly mirrored GRF9 expression determined in transcriptome studies using tiling arrays: GRF9 expression was high in leaves with proliferating cells while it gradually decreased when elemental expansion, also known as surface extension , became prominent . GRF9 is also expressed in flowers (here mostly in the carpels), the abscission zone of siliques, and in roots. In these tissues as well as in developing leaves, GRF9 expression might be finely tuned by miR396 (see below).
GRF9 restricts cell proliferation in the incipient leaf primordium
We employed reverse genetics approaches to reveal the functional importance of GRF9 in leaf development. Loss-of-function grf9 mutants had bigger rosette leaves and petals than WT while plants overexpressing GRF9 produced smaller leaves and petals by affecting cell numbers but not cell sizes. Bigger leaves were previously reported for one of the grf9 mutants studied here (grf9-1) and the phenotype of it observed in this study is in accordance with previous results [22,67], although Horiguchi et al. (2005)  did not find the increase in leaf size in grf9 to be significant. Although several members of the GRF family in Arabidopsis positively determine final leaf size by affecting cell proliferation or elemental expansion [21–24], we demonstrate here that GRF9 negatively regulates leaf size dimensions by inhibiting cell proliferation in the incipient leaf primordium and the developing leaf which might affect the position of the cell cycle arrest front (see Fig 8). The increased size of the incipient leaf primordium in the grf9-2 mutant occurred without a change in the size of SAM or cell sizes, suggesting a higher cell proliferation rate in grf9-2 during the initial phase of leaf establishment which is supported by a considerably higher expression of HISTONE4 and CYCB1;1 in grf9-2 than WT primordia (Fig 2E and 2F and S5 Fig).
(A) GRF9 restricts the size of the incipient leaf primordium at the shoot apex, whitout affecting cell size or the size of the SAM. While leaf primordium size is increased in grf9 mutants, compared to wild type (WT), it trends to be smaller in GRF9 overexpressor (GRF9ox) plants. Similarly, cell numbers in young developing leaves are bigger in grf9, but smaller in GRF9ox plants, in accordance with a higher number of cells in the developing grf9 leaves, potentially contributing to the position of the arrest front. (B) Gene regulatory network by which GRF9 and ORG3 influence leaf size. MiR396 targets GRF9 transcript and negatively regulates its abundance. GRF9 interacts with GIF1 which, similar to other GRFs, influences leaf size determination. ORG3 expression is positively regulated by GRF9 and OBP3, but repressed by the TCP20 transcription factor . Finally, ORG3 negatively regulates cell proliferation thereby directly influencing leaf size. For more details, see text.
One of the most accurate ways of identifying actively proliferating cells is to directly label newly synthesized DNA in the dividing cells e.g. using 5-ethynyl-2'-deoxyuridine (EdU) which has a structure similar to that of thymidine thereby facilitating its incorporation into newly synthesized DNA molecules [56,58,61]. EdU staining has been successfully employed in Arabidopsis for the determination of actively proliferating cells in the leaf primordium as well as in the quiescent centre (QC) of roots [44,68]. By employing the EdU incorporation assay we here show that grf9 knockout mutants have significantly more proliferating cells than the wild type, while the number of proliferating cells is slightly reduced in GRF9ox lines (Fig 4). Thus, GRF9 determines final leaf size by affecting the number of cells within the incipient leaf primordium and thereafter the number of cells in young leaves. GRF9 might exert its function by restricting the cell proliferation process in developing leaves or by reducing the number of leaf founder cells which has not been investigated here.
It has been suggested that miR396, which inhibits various GRFs, contributes to the movement of the AF in the developing leaf . Vice versa, GRFs can regulate miR396 expression ; one may, therefore, speculate that overexpression of GRF9 can synergistically regulate miR396 expression and antagonistically regulate other GRFs, resulting in fewer cells in the developing leaf. Furthermore, as GRF9 harbours a GRF9 binding site in its promoter, there is the further possibility that it autoregulates its own expression; whether this is indeed happening was however not tested here.
Previously, Wu et al. (2014) reported that ZmGRF10 (Zea mays GRF10) negatively regulates cell numbers and leaf size in maize ; interestingly, ZmGRF10 belongs to the same phylogenetic class as AtGRF9 but is different from other GRFs which act as positive regulators of leaf size . A model was proposed in which the homeostasis of GRF/GIF (GRF-INTERACTING FACTOR) complexes regulates cell proliferation in maize leaves where this homeostasis is adjusted by ZmGRF10 as a negative, and ZmGRF1 as a positive regulator [34,45]. Horiguchi et al. (2005) also showed in Arabidopsis that the GRF5/GIF1 complex is required for establishing a proper leaf size by promoting cell proliferation activity in the leaf primordium . These authors showed, by yeast two-hybrid analysis, that GRF9 interacts with GIF1 and it may therefore be speculated that the same type of regulation exists for GRF9 although it functions as a negative regulator of cell proliferation.
The previous reports as well as our data suggest that GRF9 functions different from the other members of the GRF family in Arabidopsis, which might be due to its unique protein structure harboring two WRC domains while most other GRFs have only one such domain [21,65,70,71]. Currently, the molecular significance of the presence of two WRC domains in some plant GRF proteins remains unknown. Moreover, AtGRFs harbor the conserved QLQ domain which, however, within the Arabidopsis proteins is unique in GRF9 where a leucine is replaced by phenylalanine , althougt this does not affect its interaction with GIF1 [22,41]. Interestingly, it has been shown that other members of the GIF family in Arabidopsis, namely GIF2 and GIF3, interact with all GRFs except GRF9 . Whether this is due to the presence of two WRC domains in GRF9 needs to be investigated further. One possible mode of action is that GRF9 contributes to locate the cell cycle arrest front (AF) by controlling the transition from cell proliferation to cell elongation. This model is consistent with the fact that expression of GRF9 is restricted to the proximal part of the young growing leaf while it fades towards the AF and further supported by the observation that the AF is shifted to a more distal part of the leaf blade when GRF9 is knocked out.
Using in vitro binding site selection, we identified the six-base motif 5'-CTGACA-3' as the core binding site of GRF9 (Fig 5A). This binding site resembles that of GRF7 (TGTCAGG) . Another study has shown that a short sequence enriched in CTG or CAG residues contains the binding site for Oryza sativa GRF3 (OsGRF3) and OsGRF10 . The authors also showed that GRF4, 5 and 6 from Arabidopsis bind to this short sequence and concluded that those are conserved motifs in mono- and dicots. Our results support this model.
A GRF9 –ORG3 regulatory cascade
We identified several potential target genes of GRF9, one of which is OBP3-RESPONSIVE GENE3 (ORG3; S1 Table). qRT-PCR analysis revealed downregulation of ORG3 expression in grf9 mutants, and enhanced expression in GRF9 overexpressors (S8 Fig). Using a luciferase-based transactivation assay in Arabidopsis mesophyll cell protoplasts, we showed that GRF9 activates ORG3 (Fig 5F). Moreover, in vitro (EMSA) as well as in vivo (ChIP) analyses revealed direct binding of GRF9 to the ORG3 promoter (Fig 5B and 5E).
Here, in our study, loss-of-function of ORG3 resulted in bigger rosette leaves with an increased number of cells compared to WT, while cell sizes remained unchanged, similar to grf9. Similar to our study, Van Dingenen et al. (2017)  reported bigger leaves of the org3-1 (bhlh39) mutant, compared to WT, due to an increase in leaf pavement cell number.
To substantiate our finding that knocking out ORG3 triggers the formation of bigger leaves, we tested a second knockout mutant (org3-2) and made the same observation while overexpression of ORG3 resulted in smaller leaves (Fig 6). Our data thus strongly suggest that ORG3, like its upstream regulator GRF9, functions as a negative regulator of leaf growth. These data, together with the genetic interaction studies, demonstrate that GRF9 and ORG3 establish a previously unknown regulatory cascade to control leaf size (Fig 8).
Moreover, norflurazon (NF), a chemical inhibitor of retrograde signaling and chloroplast differentiation, causes both, a delay in the transition from cell proliferation to elemental expansion and differentiation processes; plants treated with NF had an increased cell proliferation area and the position of the arrest front was closer to the leaf tip , similar to what we observed here for the grf9 mutant. Of note, expression of ORG3 is strongly reduced in NF-treated plants. In untreated plants, ORG3 shows maximal expression at days 9 and 10, i.e. when the transition of cell proliferation to elemental expansion occurs, while expression decreases thereafter, in accordance with the model that ORG3 contributes to establishing the cell cycle arrest front during leaf development .
Stress- and ABA-related genes are among the GRF9 early responsive genes
Gene expression profiling revealed a high number of stress- and ABA-related genes among the genes differentially expressed upon induction of GRF9 expression (S1 Table). It has been reported that other members of this family, including GRF1, GRF3 and GRF7, play important roles in the coordination of plant growth with stress responses [38,39,51]. We checked the list of differentially expressed genes in the GRF9-IOE datasets and publically available transcriptome data from plants overexpressing miR396-resistant versions of GRF1 (rGRF1ox) and GRF3 (rGRF3ox), both producing bigger leaves than WT like the grf9 mutants, as well as of the grf1/2/3 triple mutant, producing smaller leaves , like GRF9 overexpressors. While only two genes repressed in GRF9-IOE where induced in rGRF1ox or rGRF3ox (S2 Table), 36 of the 94 genes (38%) regulated in GRF9-IOE are also similarily regulated in the grf1/2/3 triple mutant (S2 Table) including SAP12, ZAT6, ZAT10, ZAT11, ZAT12, WRKY40, WRKY48, WRKY54, ORE1 and several other genes that have a role in stress responses and ABA signalling [74–84]. Of note, the stress hormone ABA may function as an important factor in determining organ size [85–87], indicating that GRF9 plays a role in coordinating growth with stress responses as suggested for some other members of the GRF family [38,39]. Among the genes down-regulated in the GRF9-IOE line are ARR6 (TYPE-A ARABIDOPSIS RESPONSE REGULATOR6) and DOT1 (DEFECTIVELY ORGANIZED TRIBUTARIES1) which have been shown to positively function in leaf growth and development [88–91].
We also compared the list of differentially expressed genes in GRF5ox plants (producing bigger leaves ) and grf7-1 (with smaller leaves ) with the genes regulated in GRF9-IOE seedlings after estradiol induction. We found only one gene, namely WRKY54, to be downregulated in GRF5ox but upregulated in GRF9-IOE plants, and 18 genes commonly upregulated in grf7-1 and GRF9-IOE plants, of which several are stress related such as WRKY40 and ETHYLENE RESPONSE FACTOR 105 (ERF105) transcription factors (S2 Table).
In conclusion, we have shown that GRF9 negatively regulates final leaf size by restricting cell proliferation predominantly in the incipient leaf primordium, and limiting cell proliferation in the young leaf, which may contribute to the positioning of the cell cycle arrest front. Another but here not investigated possibility is that GRF9 limits the number of leaf founder cells within the SAM. GRF9 acts in a transcriptional cascade together with ORG3, which it activates by directly binding to its promoter. In addition, GRF9, through the induction of ABA- and stress-responsive genes, may function in coordinating final organ size with stress responses.
Materials and methods
Standard molecular techniques were performed as described . Chemicals and reagents were obtained from Sigma-Aldrich (Deisenhofen, Germany), Fluka (Buchs, Switzerland) or Merck (Darmstadt, Germany). Molecular biological reagents and kits were purchased from the suppliers indicated as well as from Roche (Mannheim, Germany) and Macherey-Nagel (Düren, Germany). Oligonucleotides were synthesized by MWG (Ebersberg, Germany) or GeneWorks (Adelaide, Australia). DNA sequencing was performed by MWG and GeneWorks. For sequence analysis, we employed the tools provided by the National Centre for Biotechnology Information (http://www.ncbi.nlm.nih.gov/) and the Arabidopsis Information Resource (TAIR; http://www.Arabidopsis.org/). Sequences of oligonucleotides used for making DNA constructs, for performing PCR, ChIP, and EMSA, and for genotyping are given in S3 Table. Data underlying figures and supplemental figures are given in S4 Table.
Plant material and growth conditions
Arabidopsis thaliana (L.) Heynh., accession Col-0, was used as the wild-type control in all experiments. The grf9-1 (SALK_140746c) and grf9-2 (SAIL_324_G07) and org3-1 (SALK_025676) and org3-2 (SAIL_737_H11) mutants were obtained from the Nottingham Arabidopsis Stock Centre (NASC; http://arabidopsis.info). T-DNA insertions and genotypes were confirmed by PCR amplification using specific primers as described in the SIGnAL database (http://signal.salk.edu).
After imbibition, the seeds were stratified at 4°C for 3 days. The seeds were germinated at 22°C under a 16-h day (140 μmol m-2 s-1) / 8-h night regime. For histochemical GUS staining and hormone treatment assays, seeds were surface-sterilized for 15 min in 70% [v/v] ethanol and then in sterilisation solution (6% [w/v] sodium hypochlorite) for 10 min and thereafter washed three times with autoclaved ddH2O. After sterilization, the seeds were sown on half-strength MS medium (Murashige and Skoog, 1962), supplemented with 1% (w/v) sucrose and appropriate antibiotics, and solidified with 0.7% (w/v) phytoagar. Two-week-old Arabidopsis seedlings were carefully removed from plates and transplanted to soil (Einheitserde GS90; Gebrüder Patzer, Sinntal-Jossa, Germany) or, if necessary, directly subjected to various treatments. Unless otherwise indicated, Arabidopsis plants were grown in controlled conditions in a growth chamber with 16-h day length provided by fluorescent light at 80 or 120 μmol m-2 s-1, a day/night temperature of 20/16°C and relative humidity of 60/75%.
GRF9-CELD: The GRF9 coding sequence (CDS) was PCR-amplified from Arabidopsis seedling cDNA using primers GRF9-CELD-fwd and GRF9-CELD-rev and inserted into pJET1.2 (Fermentas, Germany) from where it was then transferred via NheI and BamHI sites into plasmid pTacLCELD6XHis  to create a GRF9-CELD in-frame fusion construct (pTacGRF9LCELD6XHis). ProGRF9-FLuc: The ~1.5-kb GRF9 promoter (upstream of the translation start codon) was amplified by PCR from Arabidopsis genomic DNA and inserted into pENTR/D-TOPO vector using the pENTR Directional TOPO Cloning Kit (Invitrogen, Germany). The sequence-verified promoter was then transferred to the p2GWL7.0 vector (Ghent University; http://gateway.psb.ugent.be/vector) harbouring the firefly luciferase (FLuc) coding region by LR recombination to generate ProGRF9-FLuc (full-length GRF9 promoter). Pro35S:GRF9-GFP: the GRF9 CDS without its stop codon was amplified by PCR and inserted into the pENTR/D-TOPO vector using the pENTR Directional TOPO Cloning Kit (Invitrogen, Germany). The sequence-verified CDS was then transferred to the pK7FWG2 vector  by LR recombination. ProGRF9:GUS: a ~1.5-kb fragment upstream of the GRF9 translation initiation codon was amplified from genomic Arabidopsis Col-0 DNA by PCR using primers PGRF9-fwd and PGRF9-rev, inserted into pENTR/D-TOPO vector using the pENTR Directional TOPO Cloning Kit (Invitrogen, Germany). The sequence-verified CDS was then transferred to the pKGWFS7,0 vector . Pro35S:GRF9 and Pro35S:ORG3: the GRF9 and ORG3 CDSs, respectively, were amplified by PCR from Arabidopsis seedling cDNA, inserted individually into vector pJET1.2 (Fermentas), and then cloned via added PmeI and PacI sites into a CaMV 35S-containing pGreen0229 vector (http://www.pgreen.ac.uk/). GRF9-IOE: the GRF9 CDS was amplified by PCR from Arabidopsis seedlings cDNA using primers GRF9-IOE-fwd and GRF9-IOE-rev, inserted into pJET1.2 (Fermentas) and then cloned via XhoI and PacI sites into pER8 vector  Agrobacterium tumefaciens strains GV3101 (pMP90) was used for Arabidopsis thaliana (Col-0) transformations.
In vitro binding-site selection
GRF9-CELD fusion protein was prepared essentially as described by Xue (2005) , except that the following buffer for preparation and storage of GRF9-CELD protein was used: 10 mM sodium phosphate, pH7.2, 50 mM KCl, 0.5 mM DTT and 10 μM ZnCl2. The standard procedure for in vitro binding-site selection using Ni-NTA magnetic beads as an affinity matrix was used for selection of GRF9 binding sites , using a biotin-labelled double-stranded oligonucleotide containing a 30-nt random sequence [5’-CCAGGTGCGCTGGCGGACG(N30)GCTAGCCGATCGGAGCTCGG], except that MgCl2 in DNA-binding buffer and washing buffer was replaced with 10 μM and 1 μM ZnCl2, respectively. The GRF9-selected oligonucleotides after the sixth selection round were cloned and analysed for GRF9 binding activity. Positive clones were used for sequence analysis.
GRF9 binding assay
The DNA-binding activity of GRF9-CELD was measured essentially as described previously [63,95] using streptavidin-coated 96-well plate and a binding buffer of 25 mM HEPES/KOH, pH 7.0, 50 mM KCl, 0.5 mM DTT and 10 μM ZnCl2, 0.15 μg μl-1 sheared herring sperm DNA, 0.3 mg ml-1 bovine serum albumin, 10% [w/v] glycerol and 0.025% [v/v] Nonidet P-40. 40,000 fluorescent units h-1 of the CELD activity of GRF9-CELD protein and 2 pmol of biotinylated probes were used per assay. The washing buffer contained 25 mM HEPES/KOH, pH 7.0, 50 mM KCl and 1 μM ZnCl2. The cellulase activity of GRF9-CELD protein bound to immobilised biotinylated probes was assayed by incubation in 100 μl of the CELD substrate solution (1 mM methylumbelliferyl β-D-cellobioside (MUC) in 50 mM Na-citrate buffer, pH 6.0) at 40°C for 3 h. A biotin-labelled double-stranded oligonucleotide without a GRF9 binding site was used as a control for background activity.
Gene expression analysis by microarray hybridisation
Two micrograms of quality-checked total RNA obtained from either 2-week-old GRF9-IOE seedlings grown on MS medium (3 and 4 h after induction with 10 μM estradiol or 0.15% [v/v] ethanol for control) or detached mature leaves from 4-week-old soil-grown GRF9-IOE plants (6 h after 10 μM estradiol treatment or 0.15% [v/v] ethanol for control) were used for Affymetrix ATH1 micro-array hybridisations (one biological replicate each). Labelling, hybridisation, washing, staining, and scanning procedures were performed by ATLAS Biolabs (Berlin, Germany). Up-/down-regulated genes at each time point were obtained by calculating the ratio of the gene expression values in treatment versus control values. In addition, all time points were considered as three replicates and the differentially expressed genes were obtained using the limma package  in R (R Core Team, 2013). Expression data (GRF9-IOE-3h, GRF9-IOE-4h and GRF9-IOE-6h datasets) have been submitted to the NCBI Gene Expression Omnibus (GEO) repository (www.ncbi.nlm.nih.gov/geo/) and are available under accession number GSE98490.
Quantitative RT-PCR was performed as previously described  using RNA extracted from 2-week-old GRF9-IOE seedlings grown on MS medium 1, 2, 3, 5 and 6 h after induction with 10 μM estradiol (or 0.15% [v/v] ethanol for control), or from 2-week-old GRF9ox and grf9-1 seedlings grown on MS medium, by RNeasy Plant Mini Kit (Qiagen, Hilden, Germany). RNA was extracted from different tissues or whole seedlings (at least three biological replicates). Genomic DNA contamination was removed from RNA using Turbo DNA Free Kit (Ambion/Thermo Fisher Scientific, Darmstadt, Germany) and cDNA was synthesized by RevertAid First Strand cDNA Synthesis Kit using oligo(dT) primer (Thermo Fisher Scientific, Sankt-Leon Rot, Germany). Primers were designed using the QuantPrime tool (; http://www.quantprime.de/). PCR reactions were run on an ABI PRISM 7900HT sequence detection system (Applied Biosystems), and the amplification products were visualized using SYBR Green (Applied Biosystems). Data were normalized against reference gene ACTIN2 (At3g18780), and calculated using the ΔΔCt method . Transcript levels are calculated as the difference between an arbitrary value of 40 and dCt, so that high 40-dCt value indicates high gene expression level. Relative expression shown in Figs 1B and 3C was calculated by dividing gene expression values of grf9-2 or GRF9ox1 by those of WT, respectively.
The level of mature miR396 was determined as reported [100,101], with some modifications. In brief, RNA was extracted using TRIzol reagent (Invitrogen/Thermo Fisher Scientific, Sankt-Leon Rot, Germany) and genomic DNA contamination was removed from extracted RNA using Turbo DNA Free Kit (Ambion/Thermo Fisher Scientific, Darmstadt, Germany). cDNA was synthesized from 5 μg total RNA by SuperScript II reverse transcriptase (Invitrogen/Thermo Fisher Scientific, Sankt-Leon Rot, Germany) employing a mixture of oligo(dT) and stem-loop primers according to the instruction manual. PCR reactions were run on an ABI PRISM 7900HT sequence detection system (Applied Biosystems) using primers specific for miR396, GRF9 and ACTIN2 (S3 Table), and the amplification products were visualized using SYBR Green master mix (Applied Biosystems). Data normalization was done as explained in the previous paragraph.
Total RNA was extracted from ORG3 transgenic and WT plants and genomic DNA contamination was removed using Turbo DNA Free Kit (Ambion/Thermo Fisher Scientific, Darmstadt, Germany). cDNA was synthesized by RevertAid First Strand cDNA Synthesis Kit (Thermo Fisher Scientific). RT-PCR was performed using ORG3-specific primers in a 25-μl reaction volume containing 1 μl cDNA, 2.5 μl 10 x DreamTag Green buffer (Thermo Fisher Scientific), 0.2 mM dNTPs, 1 μM each primer, and 1 U DreamTag DNA polymerase (Thermo Fisher Scientific). The PCR cycling program was as follows: initial denaturation of 1 min at 95°C, followed by 25 cycles of 95°C for 30 s, 57°C for 30 s and 72°C for 1 min. The final extension phase was 10 min at 72°C. ACTIN2-specific primers were used for control amplifications.
Whole leaves and leaf cells were observed with a stereoscopic microscope (Lumar, Carl Zeiss, Jena, Germany) and a Nomarski differential interference contrast microscope (BX51, Olympus, Tokyo, Japan), respectively. For histological analysis of cells, the first set of leaves from 20-day-old plants were collected. The leaves were fixed in FAA (formalin: acetic acid: ethanol, 1: 1: 18) and cleared using chloral hydrate solution (chloral hydrate 100 g, glycerol 10 g, water 25 ml), as described before . Whole leaves and cells were observed as previously described . Means ± SD from at least eight individual plants are given in the figures. To calculate the total cell number in leaves, we measured cell density of observed images of cells, and multiplied the cell density by the area of the same leaf. Kinetic analyses were performed as described .
Size of cells in leaf primodia and cell number in the layer 1 (L1) of the SAM were analysed in Fiji (https://fiji.sc/) using images generated with a Nikon eclipse E600 microscope. Means ± SEM from at least eight individual plants are given in the figures.
Visualization of cell proliferating with 5-ethynyl-2'-deoxyuridine (EdU)
To detect proliferating cells, we used the EdU assay, which stains S-phase cells . Five-day-old-seedlings were incubated with 10 μm EdU (Invitrogen, cat no: A10044; dissolved in water) for 4 h under illumination in a culture chamber. After incubation, samples were fixed in 90% [v/v] acetone for 10 min, washed twice with phosphate buffered saline (PBS) buffer (pH 7.0). Subsequently, the buffer was replaced with FAA and incubated under vacuum for 2 h. Fixed seedlings were washed twice with 0.5% [v/v] Triton X-100 in PBS for 5 min each, then washed again with PBS for 5 min. Next, samples were incubated in EdU detection cocktail (10 μm Alexa 488, Invitrogen; 100 mM Tris-HCl, pH 8.5, 1 mM CuSO4, 100 mM ascorbate) for 30 min. Finally, samples were rinsed three times with PBS for 20 min each, then transferred onto microscopy slides and covered with a chloral hydrate solution to make the samples transparent. Observations were done using a confocal laser scanning microscope (LSM 710; Zeiss, Jena, Germany). EdU signals were scanned and calculated by ImageJ (http://imagej.nih.gov/ij/).
Tissue embedding, sectioning and RNA in situ hybridization
Meristems of 2-day-old WT and GRF9 transgenic plants grown in long days (16 h light/8 h dark) were harvested, fixed, embedded into wax using an automated tissue processor (ASP200S; Leica, Wetzlar, Deutschland) and embedding system (HistoCore Arcadia; Leica). Sections of 8 μm thickness were prepared using a rotary microtome (RM2255; Leica). Briefly, RNA in situ hybridization was carried out by dewaxing slides containing sections in Histoclear solution (Biozym Scientific, Hessisch Oldendorf, Germany) and processed through ethanol series. Then, the slides were incubated in Proteinase K (Roche, Mannheim, Germany) and dehydrated by processing through an ethanol series. Further, HISTONE4 (H4) or CYCB1;1 antisense probes mixed with hybridisation buffer were applied to the slides and hybridized overnight. The H4 and CYCB1;1 probes were amplified and cloned into pGEM-T Easy Vector (Promega, Madison, Wisconsin, USA) and synthesized with the DIG RNA Labeling Kit (Roche). After the hybridization overnight, slides were washed out and incubated with 1% blocking reagent (Roche) in 1 × TBS /0.1% Triton X-100. For immunological detection, the Anti-DIG antibody (Roche) solution diluted 1:1,250 in blocking reagent was applied to the slides. Then, the slides were washed and for the colorimetric detection, the NBT/BCIP stock solution (Roche) diluted 1:50 in 10% polyvinyl alcohol (PVA) in TNM-50 was applied to the slides. The slides were incubated overnight and imaged with a Nikon eclipse E600 microscope (Nikon, Dűsseldorf, Germany) using NIS-Elements BR 4.51.00 software (Nikon). The figure panel was generated in Adobe Photoshop CS5 (Adobe Systems, San Jose, USA).
For toluidine blue staining slides were dewaxed by incubating in Histoclear and an ethanol series: 100% EtOH for 2 min, 100% EtOH for 2 min, 95% EtOH for 1 min, 90% EtOH for 1 min, 80% EtOH for 1 min, 60% EtOH + 0.75% of NaCl for 1 min, 30% EtOH + 0.75% of NaCl for 1 min, 0.75% NaCl for 1 min, and PBS for 1 min. The slides were shortly left to dry at 42°C and then incubated in 0.01% toluidine blue/sodium borate solution for 2 min, briefly washed with water and 80% EtOH. The sections were imaged as described above.
Rosette growth analysis using a phenotyping platform
To perform whole-rosette phenotyping (S4A and S4B Fig), we used a growth phenotyping pipeline previously established . To this end, Col-0, grf9-2 and GRF9ox-1 were sown in 5-cm-diameter pots in a 54-pot tray (QuickPot 54R, HerkuPlast-Kubern, Ering am Inn, Germany; http://www.herkuplast.com). Plants were grown in growth cabinets with a tightly controlled environment (Percival Scientific Inc., Perry, IO, USA http://www.percival-scientific.com) at 22°C and 70% relative humidity during the day, 18°C and 80% humidity at night, at a 12 h day: 12 h night cycle (equal day), or an 8 h day: 16 h night cycle (short day). Homogenized stratification was maximized by keeping the seeds for uniform germination at 6°C and 80% humidity for the first 7 nights (day condition was the same as indicated before). Developmental stages were defined as reported . Images were captured by a robot arm holding a camera of the Scanalyzer HTS instrument (LemnaTec, Wuerselen, Germany, http://www.lemnatec.com). Image analysis was performed using LemnaGrid (provided with the image capturing system) and growth analysis was done using the growth phenotyping pipeline .
Electrophoretic mobility shift assay (EMSA)
EMSA was performed with GRF9-CELD fusion protein as described previously [107,108] using 5'-DY682-labelled oligonucleotides harbouring the GRF9 BS (5'-CTGACA-3'). Oligonucleotides were purchased from MWG Eurofins Genomics (Ebersberg, Germany).
Isolation and transformation of Arabidopsis mesophyll cell protoplasts were done based on the tape-sandwich method . Assays were performed as described , using Pro35S:GRF9 effector plasmid. Luciferase activity was determined using the Dual-Luciferase Reporter Assay System (Promega, Germany) and a GloMax 96 microplate luminometer (Promega, Germany). All tests were performed in three biological replications with five technical replications per assay.
Five-day-old Arabidopsis seedlings expressing GFP-tagged GRF9 protein from the CaMV 35S promoter (Pro35S:GRF9-GFP) were used for ChIP-qPCR. ChIP was done as reported . μMACS GFP Isolation Kit (Miltenyi, Germany) was used for immunopurification of GRF9-GFP-DNA complex. qPCR was performed using primers flanking the GRF9 binding site of the ORG3 promoter. Primers detecting enrichment of a promoter region lacking GRF9 binding site (At2g22180) was used for negative control. The relative enrichment was calculated by the comparative cycle threshold method . The amounts of immunoprecipitated DNA were normalized to the input fraction. To calculate fold enrichment, normalized ChIP signals were compared between Pro35S:GRF9-GFP and wild-type plants as control , where the ChIP signal is given as the fold increase in signal relative to the background signal.
S1 Table. Genes affected in GRF9-IOE lines after EST induction and comparison with other GRF9-modified plants.
S2 Table. GRF9-responsive genes in GRF9-IOE seedlings compared to differentially expressed genes in other publically available AtGRF transcriptomes.
S4 Table. Data corresponding to Figures and Supplemental Figures.
S1 Fig. Analysis of GRF9 promoter-driven reporter activity in ProGRF9:GUS lines.
(A)–(D) Histochemical GUS staining of GRF9 expression pattern in leaves of 4-, 6-, 8-, and 12-day-old seedlings, respectively. (E) and (F) Leaves of 3-week-old plants. Note the expression of GRF9 in the cell proliferation zone of very young leaves (B, C) and the vascular tissue of older leaves (D—F). (G) and (H) Main and lateral roots. (I)–(L) Flowers at different developmental stages. Note, that younger flowers show stronger GUS activity. (M)–(P) Siliques at different developmental stages.
S2 Fig. Expression of GRF9 determined by qRT-PCR.
(A) GRF9 expression in different tissues of 40-day-old WT plants. (B) GRF9 expression in 2-week-old WT seedlings treated with different concentrations of auxin (in the form of 2,4-D) or cytokinin (in the form of zeatin). (C) Histochemical GUS staining of GRF9 expression pattern in young Arabidopsis Col-0 seedlings treated with auxin (in the form of 2,4-D) or cytokinin (in the form of zeatin). Values in panels A and B represent the means ± SD of three technical replicates from two biological replicates.
S3 Fig. Genotyping of grf9-1 and grf9-2 mutants.
(A) grf9-1 (SALK_140746c) and (B) grf9-2 (SAIL_324_G07). (a) Right gene-specific primer and T-DNA left border primer, and (b) left and right gene-specific primers for genotyping (designed by http://signal.salk.edu/tdnaprimers.2.html). M, DNA size marker. Primer sequences are given in S3 Table.
S4 Fig. Rosette growth of GRF9 transgenic lines under different light regimes.
Rosette phenotype of grf9-2 and GRF9ox1 in comparison to WT plants in (A) short day (8 h light / 16 h dark) and (B) equal day (12 h light / 12 h dark) conditions, determined using a LemnaTec phenotyping platform . Note the more pronounced phenotype of the grf9 mutant in short-day condition. (C) Rosette area determined at 21 days after sowing (DAS) for short-day-grown plants, and at 23 DAS for plants grown in equal day/night length. Values represent means ± SD of at least 50 plants each. Asterisks indicate significant difference from the WT (Student's t-test; p < 0.05).
S5 Fig. RNA in situ hybridization using the CYCLIN B1;1 (CYCB1;1) probe.
In situ hybridization was done on longitudinal sections of the shoot apical meristem with leaf primordia of WT and grf9-2 plants (Scale bar 100 μm).
S6 Fig. Petal phenotype of grf9 and GRF9ox plants.
(A) Mature flowers and petals of WT, grf9-1, grf9-2 and GRF9ox1 plants. (B) Petal size and (C) petal cell area. Data represent means ± SD from at least 32 petals (i.e., 4 petals from at least 8 plants). Asterisks indicate a significant difference from the WT (Student's t-test; p < 0.05). Scale bars = 1 mm (panel A, top) and 0.5 mm (panel A, bottom).
S7 Fig. Base substitution analysis of the GRF9 binding site.
The experiment was performed to define the DNA-binding sequence specificity of GRF9 by base substitution mutagenesis. Biotin-labelled double-stranded oligonucleotides were used. Bases that were substituted are shown in bold and as lower-case letters. The values for GRF9 binding activity are shown on the right and are means ± SD of three independent assays, relative to the binding activity of GRFE1 (1,778 fluorescence units per h produced by the CELD activity of GRF9-CELD fusion protein). The core GRF9 binding sequence defined by this analysis is CTGACA.
S8 Fig. Expression of 23 GRF9 early responding genes in different GRF9-modified lines.
Gene expression as determined by Affymetrix ATH1 microarray hybridizations (first two columns) or qRT-PCR (other columns). RNA for expression analysis was obtained from 2-week-old GRF9-IOE seedlings grown on MS medium and induced with 10 μM estradiol for the indicated time points (0.15% [v/v] ethanol as control), or from 2-week-old GRF9ox and grf9-1 seedlings grown on MS medium (WT as control). Values represent the means of replicates obtained from three sets of seedlings (except for the microarray data where each value represents one replicate).
S9 Fig. Genotyping and expression analysis in GRF9- and ORG3-modified lines.
Genotyping of (A) org3-1 (SALK_025676) and (B) org3-2 (SAIL_737_H11) mutants. (a) Right gene-specific primer and T-DNA left boarder primer, and (b) left and right gene-specific primers for genotyping (designed by http://signal.salk.edu/tdnaprimers.2.html). M, DNA size marker. Primer sequences are given in S3 Table. (C) Semi-quantitative RT-PCR using ORG3-specific primers performed on total RNA isolated from 1-week-old org3-1, org3-2, WT, ORG3ox1 and ORG3ox2 seedlings. ACTIN2 was used as a control. (D) Expression of ORG3 measured by qRT-PCR in org3 knockout and ORG3ox plants. (E) Expression of GRF9 and ORG3 measured by qRT-PCR in grf9-2 org3-1 (lines 3 and 7) and GRF9ox-1 org3-1 (lines 33 and 34) double mutants. Values in panels D and E represent the means of three technical replicates ± SD. (F) DNA genotyping results of double mutant lines using (a) right gene-specific primer and T-DNA left boarder primer, (b) left and right gene-specific primers for genotyping (designed by http://signal.salk.edu/tdnaprimers.2.html), and (c) 35S-up and reverse GRF9-IOE specific primers. Genes tested by the chosen primer combinations are underlined. M, DNA size marker.
S10 Fig. Petal phenotype of the org3-1 mutant.
(A) Mature petals of WT and org3-1 plants. (B) Petal size and (C) petal cell area. Data represent means ± SD from at least 32 petals (i.e., 4 petals from at least 8 plants). The asterisk indicates a significant difference from WT (Student's t-test; p < 0.05). Bar = 0.5 mm.
We thank Luiz Gustavo Guedes Corrêa for scientific discussions, Samuel Arvidsson for help with rosette phenotyping and scientific discussions, Nooshin Omranian for support of data analyses, Krzysztof Brzezinka for help in ChIP experiments, Eike Kamann for cloning constructs for RNA in situ hybridizations, and Christopher Wills for suggestions and scientific discussions regarding EMSA experiments.
- 1. Marcotrigiano M. A role for leaf epidermis in the control of leaf size and the rate and extent of mesophyll cell division. Am J Bot. 2010; 97:224–33. pmid:21622382
- 2. Kawade K, Horiguchi G, Tsukaya H. Non-cell-autonomously coordinated organ size regulation in leaf development. Development. 2010; 137:4221–7. pmid:21068059
- 3. Gonzalez N, Vanhaeren H, Inzé D. Leaf size control: complex coordination of cell division and expansion. Trends Plant Sci. 2012; 17:332–40. pmid:22401845
- 4. Hepworth J, Lenhard M. Regulation of plant lateral-organ growth by modulating cell number and size. Curr Opin Plant Biol. 2014; 17:36–42. pmid:24507492
- 5. Donnelly PM, Bonetta D, Tsukaya H, Dengler RE, Dengler NG. Cell cycling and cell enlargement in developing leaves of arabidopsis. Dev Biol. 1999; 215:407–19. pmid:10545247
- 6. Breuninger H, Lenhard M. Control of tissue and organ growth in plants. Curr Top Dev Biol. 2010; 91:185–220. pmid:20705183
- 7. Andriankaja ME, Danisman S, Mignolet-Spruyt LF, Claeys H, Kochanke I, Vermeersch M, et al. Transcriptional coordination between leaf cell differentiation and chloroplast development established by TCP20 and the subgroup Ib bHLH transcription factors. Plant Mol Biol. 2014; 85:233–45. pmid:24549883
- 8. Das Gupta M, Nath U. Divergence in patterns of leaf growth polarity is associated with the expression divergence of mir396. Plant Cell. 2015; 27:2785–99. pmid:26410303
- 9. Nelissen H, Gonzalez N, Inzé D. Leaf growth in dicots and monocots: so different yet so alike. Curr Opin Plant Biol. 2016; 33:72–6. pmid:27344391
- 10. Green PB. Growth and cell pattern formation on an axis: critique of concepts, terminology, and modes of study. Bot Gaz. 1976; 137:187–202.
- 11. Ferjani A, Horiguchi G, Yano S, Tsukaya H. Analysis of leaf development in fugu mutants of arabidopsis reveals three compensation modes that modulate cell expansion in determinate organs. Plant Physiol. 2007; 144:988–99. pmid:17468216
- 12. White DWR. Peapod regulates lamina size and curvature in arabidopsis. Proc Natl Acad Sci U S A. 2006; 103:13238–43. pmid:16916932
- 13. Andriankaja M, Dhondt S, De Bodt S, Vanhaeren H, Coppens F, De Milde L, et al. Exit from proliferation during leaf development in Arabidopsis thaliana: a not-so-gradual process. Dev Cell. 2012; 22:64–78. pmid:22227310
- 14. Kalve S, De Vos D, Beemster GTS. Leaf development: a cellular perspective. Front Plant Sci. 2014; 5:1–25. pmid:25132838
- 15. Kazama T, Ichihashi Y, Murata S, Tsukaya H. The mechanism of cell cycle arrest front progression explained by a KLUH/CYP78A5-dependent mobile growth factor in developing leaves of Arabidopsis thaliana. Plant Cell Physiol. 2010; 51:1046–54. pmid:20395288
- 16. Rodriguez RE, Mecchia MA, Debernardi JM, Schommer C, Weigel D, Palatnik JF. Control of cell proliferation in Aarabidopsis thaliana by microrna mir396. Development. 2010; 137:103–12. pmid:20023165
- 17. Kim JH, Tsukaya H. Regulation of plant growth and development by the GROWTH-REGULATING FACTOR and GRF-INTERACTING FACTOR duo. J Exp Bot. 2015; 66:6093–107. pmid:26160584
- 18. Anastasiou E, Lenhard M. Growing up to one’s standard. Curr Opin Plant Biol. 2007; 10:63–9. pmid:17134936
- 19. Powell AE, Lenhard M. Control of organ size in plants. Curr Biol. 2012; 22:R360–7. pmid:22575478
- 20. Rodriguez R, Debernardi J, Palatnik J. Morphogenesis of simple leaves: regulation of leaf size and shape. Wiley Interdiscip Rev Dev Biol. 2014; 3:41–57. pmid:24902833
- 21. Kim JH, Choi D, Kende H. The AtGRF family of putative transcription factors is involved in leaf and cotyledon growth in arabidopsis. Plant J. 2003; 36:94–104. pmid:12974814
- 22. Horiguchi G, Kim G-T, Tsukaya H. The transcription factor AtGRF5 and the transcription coactivator an3 regulate cell proliferation in leaf primordia of Arabidopsis thaliana. Plant J. 2005; 43:68–78. pmid:15960617
- 23. Kim JH, Lee BH. GROWTH-REGULATING FACTOR4 of Arabidopsis thaliana is required for development of leaves, cotyledons, and shoot apical meristem. J Plant Biol. 2006; 49:463–8.
- 24. Debernardi JM, Mecchia M a, Vercruyssen L, Smaczniak C, Kaufmann K, Inze D, et al. Post-transcriptional control of GRF transcription factors by microrna mir396 and GIF co-activator affects leaf size and longevity. Plant J. 2014; 79:413–26. pmid:24888433
- 25. Liu D, Song Y, Chen Z, Yu D. Ectopic expression of mir396 suppresses GRF target gene expression and alters leaf growth in arabidopsis. Physiol Plant. 2009; 136:223–36. pmid:19453503
- 26. Casadevall R, Rodriguez R, Debernardi J, Palatnik J, Casati P. Repression of growth regulating factors by the microrna396 inhibits cell proliferation by UV-b radiation in arabidopsis leaves. Plant Cell. 2013; 25:3570–83. pmid:24076976
- 27. Ercoli MF, Rojas AML, Debernardi JM, Palatnik JF, Rodriguez RE. Control of cell proliferation and elongation by mir396. Plant Signal Behav. 2016; 11:e1184809. pmid:27172373
- 28. Lee BH, Jeon JO, Lee MM, Kim JH. Genetic interaction between GROWTH-REGULATING FACTOR and CUP-SHAPED COTYLEDON in organ separation. Plant Signal Behav. 2015; 10:e988071-1–4. pmid:25761011
- 29. Kim JH, Kende H. A transcriptional coactivator, AtGIF1, is involved in regulating leaf growth and morphology in arabidopsis. Proc Natl Acad Sci U S A. 2004; 101:13374–9. pmid:15326298
- 30. Lee BH, Ko J-H, Lee S, Lee Y, Pak J-H, Kim JH. The arabidopsis GRF-INTERACTING FACTOR gene family performs an overlapping function in determining organ size as well as multiple developmental properties. Plant Physiol. 2009; 151:655–68. pmid:19648231
- 31. Ha Lee B, Hoe Kim J. Spatio-temporal distribution patterns of GRF-INTERACTING FACTOR expression and leaf size control. Plant Signal Behav. 2014; 9:1–4.
- 32. Kawade K, Horiguchi G, Usami T, Hirai MY, Tsukaya H. ANGUSTIFOLIA3 signaling coordinates proliferation between clonally distinct cells in leaves. Curr Biol. 2013; 23:788–92. pmid:23602479
- 33. Vercruyssen L, Verkest A, Gonzalez N, Heyndrickx KS, Eeckhout D, Han S-KS-K, et al. ANGUSTIFOLIA3 binds to SWI/SNF chromatin remodeling complexes to regulate transcription during arabidopsis leaf development. Plant Cell. 2014; 26:210–29. pmid:24443518
- 34. Wu L, Zhang D, Xue M, Qian J, He Y, Wang S. Overexpression of the maize GRF10, an endogenous truncated GROWTH-REGULATING FACTOR protein, leads to reduction in leaf size and plant height. J Integr Plant Biol. 2014; 56:1053–63. pmid:24854713
- 35. Debernardi JM, Rodriguez RE, Mecchia M a, Palatnik JF. Functional specialization of the plant mir396 regulatory network through distinct microrna-target interactions. PLoS Genet. 2012; 8:e1002419. pmid:22242012
- 36. Wang L, Gu X, Xu D, Wang W, Wang H, Zeng M, et al. Mir396-targeted AtGRF transcription factors are required for coordination of cell division and differentiation during leaf development in arabidopsis. J Exp Bot. 2011; 62:761–73. pmid:21036927
- 37. Bao M, Bian H, Zha Y, Li F, Sun Y, Bai B, et al. Mir396a-mediated basic helix-loop-helix transcription factor bHlH74 repression acts as a regulator for root growth in arabidopsis seedlings. Plant Cell Physiol. 2014; 6:1343–53. pmid:24793750
- 38. Hewezi T, Maier TR, Nettleton D, Baum TJ. The arabidopsis microrna396-GRF1/GRF3 regulatory module acts as a developmental regulator in the reprogramming of root cells during cyst nematode infection. Plant Physiol. 2012; 159:321–35. pmid:22419826
- 39. Liu J, Rice JH, Chen N, Baum TJ, Hewezi T. Synchronization of developmental processes and defense signaling by GROWTH REGULATING TRANSCRIPTION FACTORS. PLoS One. 2014; 9:e98477. pmid:24875638
- 40. Pajoro A, Madrigal P, Muiño JM, Matus JT, Jin J, Mecchia M a, et al. Dynamics of chromatin accessibility and gene regulation by MADS-domain transcription factors in flower development. Genome Biol. 2014; 15:R41. pmid:24581456
- 41. Liang G, He H, Li Y, Wang F, Yu D. Molecular mechanism of microrna396 mediating pistil development in arabidopsis. Plant Physiol. 2014; 164:249–58. pmid:24285851
- 42. Vercruyssen L, Tognetti VB, Gonzalez N, Van Dingenen J, De Milde L, Bielach A, et al. GROWTH REGULATING FACTOR5 stimulates arabidopsis chloroplast division, photosynthesis, and leaf longevity. Plant Physiol. 2015; 167:817–32. pmid:25604530
- 43. Nath U, Crawford BCW, Carpenter R, Coen E. Genetic control of surface curvature. Science. 2003; 299:1404–7. pmid:12610308
- 44. Ichihashi Y, Kawade K, Usami T, Horiguchi G, Takahashi T, Tsukaya H. Key proliferative activity in the junction between the leaf blade and leaf petiole of arabidopsis. Plant Physiol. 2011; 157:1151–62. pmid:21880932
- 45. Nelissen H, Eeckhout D, Demuynck K, Persiau G, Walton A, van Bel M, et al. Dynamic changes in ANGUSTIFOLIA3 complex composition reveal a growth regulatory mechanism in the maize leaf. Plant Cell. 2015; 27:1605–19. pmid:26036253
- 46. Sieberer T, Hauser M, Seifert GJ, Luschnig C, Amp MP. PROPORZ1, a putative arabidopsis transcriptional adaptor protein, mediates auxin and cytokinin signals in the control of cell proliferation. Curr Biol. 2003; 13:837–42. 10.1016/S. pmid:12747832
- 47. Werner T, Motyka V, Laucou V, Smets R, Onckelen H Van, Schmuelling T. Cytokinin-deficient transgenic arabidopsis plants show functions of cytokinins in the regulation of shoot and root meristem activity. Plant Cell. 2003; 15:2532–50. pmid:14555694
- 48. del Pozo JC, Lopez-Matas MA, Ramirez-Parra E, Gutierrez C. Hormonal control of the plant cell cycle. Physiol Plant. 2005; 123:173–83.
- 49. Inzé D, De Veylder L. Cell cycle regulation in plant development. Annu Rev Genet. 2006; 40:77–105. pmid:17094738
- 50. Sakakibara H. Cytokinins: activity, biosynthesis, and translocation. Annu Rev Plant Biol. 2006; 57:431–49. pmid:16669769
- 51. Kim J-S, Mizoi J, Kidokoro S, Maruyama K, Nakajima J, Nakashima K, et al. Arabidopsis GROWTH-REGULATING FACTOR7 functions as a transcriptional repressor of abscisic acid- and osmotic stress-responsive genes, including DREB2A. Plant Cell. 2012; 24:3393–405. pmid:22942381
- 52. Riou-Khamlichi C. Cytokinin activation of arabidopsis cell division through a D-type cyclin. Science (80-). 1999; 283:1541–4.
- 53. Riou-Khamlichi C, Menges M, Healy JMS, Murray JAH. Sugar control of the plant cell cycle: differential regulation of arabidopsis D-type cyclin gene expression. Mol Cell Biol. 2000; 20:4513–21. pmid:10848578
- 54. Colón-Carmona A, You R, Haimovitch-gal T, Doerner P. Spatio-temporal analysis of mitotic activity with a labile cyclin—GUS fusion protein. Plant J. 1999; 20:503–8. pmid:10607302
- 55. Gonzalez N, De Bodt S, Sulpice R, Jikumaru Y, Chae E, Dhondt S, et al. Increased leaf size: different means to an end. Plant Physiol. 2010; 153:1261–79. pmid:20460583
- 56. Kotogány E, Dudits D, Horváth G V, Ayaydin F. A rapid and robust assay for detection of S-phase cell cycle progression in plant cells and tissues by using ethynyl deoxyuridine. Plant Methods. 2010; 6:5. pmid:20181034
- 57. Salic A, Mitchison TJ. A chemical method for fast and sensitive detection of DNA synthesis in vivo. Proc Natl Acad Sci U S A. 2008; 105:2415–20. pmid:18272492
- 58. Vanstraelen M, Baloban M, Da Ines O, Cultrone A, Lammens T, Boudolf V, et al. APC/C-CCS52A complexes control meristem maintenance in the arabidopsis root. Proc Natl Acad Sci U S A. 2009; 106:11806–11. pmid:19553203
- 59. Qu D, Wang G, Wang Z, Zhou L, Chi W, Cong S, et al. 5-ethynyl-2’-deoxycytidine as a new agent for dna labeling: detection of proliferating cells. Anal Biochem. 2011; 417:112–21. pmid:21683679
- 60. Chehrehasa F, Meedeniya ACB, Dwyer P, Abrahamsen G, Mackay-Sim A. Edu, a new thymidine analogue for labelling proliferating cells in the nervous system. J Neurosci Methods. 2009; 177:122–30. pmid:18996411
- 61. Cavanagh BL, Walker T, Norazit A, Meedeniya ACB. Thymidine analogues for tracking DNA synthesis. Molecules. 2011; 16:7980–93. pmid:21921870
- 62. Gonzalez N, Beemster GTS, Inzé D. David and goliath: what can the tiny weed arabidopsis teach us to improve biomass production in crops? Curr Opin Plant Biol. 2009; 12:157–64. pmid:19119056
- 63. Xue G-PP. A CELD-fusion method for rapid determination of the DNA-binding sequence specificity of novel plant DNA-binding proteins. Plant J. 2005; 41:638–49. pmid:15686526
- 64. Liu H, Guo S, Xu Y, Li C, Zhang Z, Zhang D, et al. Osmir396d-regulated OsGRFs function in floral organogenesis in rice through binding to their targets OsJMJ706 and OsCR4. Plant Physiol. 2014; 165:160–74. pmid:24596329
- 65. Omidbakhshfard MA, Proost S, Fujikura U, Mueller-Roeber B. GROWTH-REGULATING FACTORs (GRFs): a small transcription factor family with important functions in plant biology. Mol Plant. 2015:1–13. pmid:25620770
- 66. Liu J, Hua W, Yang H-L, Zhan G-M, Li R-J, Deng L-B, et al. The BnGRF2 gene (GRF2-like gene from Brassica napus) enhances seed oil production through regulating cell number and plant photosynthesis. J Exp Bot. 2012; 63:3727–40. pmid:22442419
- 67. Arvidsson S, Pérez-Rodríguez P, Mueller-Roeber B. A growth phenotyping pipeline for Arabidopsis thaliana integrating image analysis and rosette area modeling for robust quantification of genotype effects. New Phytol. 2011; 191:895–907. pmid:21569033
- 68. Zhou W, Wei L, Xu J, Zhai Q, Jiang H, Chen R, et al. Arabidopsis tyrosylprotein sulfotransferase acts in the auxin/plethora pathway in regulating postembryonic maintenance of the root stem cell niche. Plant Cell. 2010; 22:3692–709. pmid:21045165
- 69. Hewezi T, Baum TJ. Complex feedback regulations govern the expression of mirna396 and its GRF target genes. Plant Signal Behav. 2012; 7:749–51. pmid:22751317
- 70. Choi D, Kim JH, Kende H. Whole genome analysis of the osgrf gene family encoding plant-specific putative transcription activators in rice (Oryza sativa l.). Plant Cell Physiol. 2004; 45:897–904. pmid:15295073
- 71. Zhang D-F, Li B, Jia G-Q, Zhang T-F, Dai J-R, Li J-S, et al. Isolation and characterization of genes encoding GRF transcription factors and GIF transcriptional coactivators in maize (Zea mays l.). Plant Sci. 2008; 175:809–17.
- 72. Kuijt SJH, Greco R, Agalou A, Shao J, ‘t Hoen CCJ, Overnäs E, et al. Interaction between the GROWTH-REGULATING FACTOR and KNOTTED1-LIKE HOMEOBOX families of transcription factors. Plant Physiol. 2014; 164:1952–66. pmid:24532604
- 73. Van Dingenen J, Antoniou C, Filippou P, Pollier J, Gonzalez N, Dhondt S, et al. Strobilurins as growth-promoting compounds: how stroby regulates arabidopsis leaf growth. Plant Cell Environ. 2017; 40:1748–60. pmid:28444690
- 74. Gechev TS, Hille J. Hydrogen peroxide as a signal controlling plant programmed cell death. J Cell Biol. 2005; 168:17–20. pmid:15631987
- 75. Balazadeh S, Wu A, Mueller-Roeber B. Salt-triggered expression of the ANAC092-dependent senescence regulon in Arabidopsis thaliana. Plant Signal Behav. 2010; 5:733–5. pmid:20404534
- 76. Benina M, Ribeiro DM, Gechev TS, Mueller-Roeber B, Schippers JHM. A cell type-specific view on the translation of mRNAs from ROS-responsive genes upon paraquat treatment of Arabidopsis thaliana leaves. Plant Cell Environ. 2015; 38:349–63. pmid:24738758
- 77. Besseau S, Li J, Palva ET. WRKY54 and WRKY70 co-operate as negative regulators of leaf senescence in Arabidopsis thaliana. J Exp Bot. 2012; 63:2667–79. pmid:22268143
- 78. Chen H, Lai Z, Shi J, Xiao Y, Chen Z, Xu X. Roles of arabidopsis WRKY18, WRKY40 and WRKY60 transcription factors in plant responses to abscisic acid and abiotic stress. BMC Plant Biol. 2010; 10:281. pmid:21167067
- 79. Pandey SP, Roccaro M, Schön M, Logemann E, Somssich IE. Transcriptional reprogramming regulated by WRKY18 and WRKY40 facilitates powdery mildew infection of arabidopsis. Plant J. 2010; 64:912–23. pmid:21143673
- 80. Davletova S, Schlauch K, Coutu J, Mittler R. The zinc-finger protein ZAT12 plays a central role in reactive oxygen and abiotic stress signaling in arabidopsis. Plant Physiol. 2005; 139:847–56. pmid:16183833
- 81. Mittler R, Kim Y, Song L, Coutu J. Gain-and loss-of-function mutations in ZAT10 enhance the tolerance of plants to abiotic stress. FEBS Lett. 2006; 580:6537–42. pmid:17112521
- 82. Nguyen XC, Kim SH, Lee K, Kim KE, Liu X-M, Han HJ, et al. Identification of a C2H2-type zinc finger transcription factor (ZAT10) from arabidopsis as a substrate of map kinase. Plant Cell Rep. 2012; 31:737–45. pmid:22134874
- 83. Rizhsky L, Davletova S, Liang H, Mittler R. The zinc finger protein ZAT12 is required for CYTOSOLIC ASCORBATE PEROXIDASE 1 expression during oxidative stress in arabidopsis. J Biol Chem. 2004; 279:11736–43. pmid:14722088
- 84. Vogel JT, Zarka DG, Van Buskirk H a, Fowler SG, Thomashow MF. Roles of the CBF2 and ZAT12 transcription factors in configuring the low temperature transcriptome of arabidopsis. Plant J. 2005; 41:195–211. pmid:15634197
- 85. Li Y, Zheng L, Corke F, Smith C, Bevan MW. Control of final seed and organ size by the da1 gene family in Arabidopsis thaliana. Genes Dev. 2008; 22:1331–6. pmid:18483219
- 86. Seifert GJ, Xue H, Acet T. The Arabidopsis thaliana fasciclin like ARABINOGALACTAN PROTEIN 4 gene acts synergistically with abscisic acid signalling to control root growth. Ann Bot. 2014; 114:1125–33. pmid:24603604
- 87. Yoshida T, Mogami J, Yamaguchi-Shinozaki K. Omics approaches toward defining the comprehensive abscisic acid signaling network in plants. Plant Cell Physiol. 2015; 56:1043–52. pmid:25917608
- 88. Kakani A. ARR5 and ARR6 mediate tissue specific cross-talk between auxin and cytokinin in arabidopsis. Am J Plant Sci. 2011; 2:549–53.
- 89. Coello P, Polacco J. ARR6, a response regulator from arabidopsis, is differentially regulated by plant nutritional status. Plant Sci. 1999; 143:211–20.
- 90. Petricka JJ, Clay NK, Nelson TM. Vein patterning screens and the defectively organized tributaries mutants in Arabidopsis thaliana. Plant J. 2008; 56:251–63. pmid:18643975
- 91. To J, Haberer G, Ferreira F. Type-A arabidopsis response regulators are partially redundant negative regulators of cytokinin signaling. Plant Cell. 2004; 16:658–71. pmid:14973166
- 92. Green MR, Sambrook J. Molecular cloning: a laboratory manual. Fourth edi. N. Y.: Cold Spring Harbor Laboratory Press; 2012.
- 93. Karimi M, Inzé D, Depicker A, Hajdukiewicz P, al. et, Hellens R., et al. GatewayTM vectors for agrobacterium-mediated plant transformation. Trends Plant Sci. 2002; 7:193–5. pmid:11992820
- 94. Zuo J, Niu QW, Chua N-HH. Technical advance: an estrogen receptor-based transactivator XVE mediates highly inducible gene expression in transgenic plants. Plant J. 2000; 24:265–73. pmid:11069700
- 95. Matallana-Ramirez LP, Rauf M, Farage-Barhom S, Dortay H, Xue G-P, Dröge-Laser W, et al. NAC transcription factor ORE1 and SENESCENCE-INDUCED BIFUNCTIONAL NUCLEASE1 (BFN1) constitute a regulatory cascade in arabidopsis. Mol Plant. 2013; 6:1432–52. pmid:23340744
- 96. Smyth GK, Ritchie M, Thorne N, Wettenhall J, Shi W. Limma: linear models for microarray data. Bioinforma. Comput. Biol. Solut. Using R Bioconductor, Springer New York; 2005, p. 397–420.
- 97. Omidbakhshfard MA, Omranian N, Ahmadi FS, Nikoloski Z, Mueller-Roeber B. Effect of salt stress on genes encoding translation-associated proteins in Arabidopsis thaliana. Plant Signal Behav. 2012; 7:1095–102. pmid:22899071
- 98. Arvidsson S, Kwasniewski M, Riaño-Pachón DM, Mueller-Roeber B. Quantprime—a flexible tool for reliable high-throughput primer design for quantitative pcr. BMC Bioinformatics. 2008; 9:465. pmid:18976492
- 99. Schmittgen TD, Livak KJ. Analyzing real-time PCR data by the comparative ct method. Nat Protoc. 2008; 3:1101–8. pmid:18546601
- 100. Chen C, Ridzon DA, Broomer AJ, Zhou Z, Lee DH, Nguyen JT, et al. Real-time quantification of micrornas by stem-loop rt-pcr. Nucleic Acids Res. 2005; 33. pmid:16314309
- 101. Soto-Suárez M, Baldrich P, Weigel D, Rubio-Somoza I, San Segundo B. The arabidopsis mir396 mediates pathogen-associated molecular pattern-triggered immune responses against fungal pathogens. Sci Rep. 2017; 7:44898. pmid:28332603
- 102. Tsuge T, Tsukaya H, Uchimiya H. Two independent and polarized processes of cell elongation regulate leaf blade expansion in Arabidopsis thaliana (L.) heynh. Development. 1996; 1600:1589–600.
- 103. Fujikura U, Horiguchi G, Tsukaya H. Dissection of enhanced cell expansion processes in leaves triggered by a defect in cell proliferation, with reference to roles of endoreduplication. Plant Cell Physiol. 2007; 48:278–86. pmid:17205970
- 104. Horiguchi G, Fujikura U, Ferjani A, Ishikawa N, Tsukaya H. Large-scale histological analysis of leaf mutants using two simple leaf observation methods: identification of novel genetic pathways governing the size and shape of leaves. Plant J. 2006; 48:638–44. pmid:17076802
- 105. Fujikura U, Elsaesser L, Breuninger H, Sánchez-Rodríguez C, Ivakov A, Laux T, et al. ATKINESIN-13A modulates cell-wall synthesis and cell expansion in Arabidopsis thaliana via the THESEUS1 pathway. PLoS Genet. 2014; 10:e1004627. pmid:25232944
- 106. Jefferson R. Assaying chimeric genes in plants: the GUS gene fusion system. Plant Mol Biol Report. 1987; 5:387–405.
- 107. Wu A, Allu AD, Garapati P, Siddiqui H, Dortay H, Zanor MI, et al. JUNGBRUNNEN1, a reactive oxygen species-responsive NAC transcription factor, regulates longevity in arabidopsis. Plant Cell. 2012; 24:482–506. pmid:22345491
- 108. Smaczniak C, Immink R, Muiño JM, Blanvillain R, Busscher M, Busscher-Lange J, et al. Characterization of MADS-domain transcription factor complexes in arabidopsis flower development. Proc Natl Acad Sci U S A. 2012; 109:1560–5. pmid:22238427
- 109. Wu F-H, Shen S-C, Lee L-Y, Lee S-H, Chan M-T, Lin C-S. Tape-arabidopsis sandwich—a simpler arabidopsis protoplast isolation method. Plant Methods. 2009; 5:16. pmid:19930690
- 110. Kaufmann K, Muiño JM, Østerås M, Farinelli L, Krajewski P, Angenent GC. Chromatin immunoprecipitation (ChIP) of plant transcription factors followed by sequencing (ChIP-SEQ) or hybridization to whole genome arrays (ChIP-CHIP). Nat Protoc. 2010; 5:457–72. pmid:20203663