The Secreted Peptide PIP1 Amplifies Immunity through Receptor-Like Kinase 7

Both animals and plants have evolved mechanisms to trigger innate immunity through perception of exogenous and endogenous molecules. In the model plant Arabidopsis thaliana, endogenous molecules such as the peptide elicitor PEP1 activate the immune response by means of cell surface-located receptors. Here we describe a new gene family in A. thaliana named prePIPs, whose members encode secreted peptide precursors, and show that one of its members, prePIP1, is secreted into extracellular space and cleaved at the C-terminus. Exogenous application of PIP1, the synthetic 13-amino acid peptide corresponding to the conserved C-terminal region of prePIP1, triggered immune responses and led to enhanced pathogen resistance in A. thaliana. We further provide evidence showing that PIP1 signals via the receptor-like kinase 7 (RLK7) and employs both shared and distinct components with the PEP1 signaling pathway. Both PIP1 and PEP1 cooperatively amplify the immune response triggered by flg22, the active epitope of bacterial flagellin.

Published in the journal: . PLoS Pathog 10(9): e32767. doi:10.1371/journal.ppat.1004331
Category: Research Article
doi: 10.1371/journal.ppat.1004331


Both animals and plants have evolved mechanisms to trigger innate immunity through perception of exogenous and endogenous molecules. In the model plant Arabidopsis thaliana, endogenous molecules such as the peptide elicitor PEP1 activate the immune response by means of cell surface-located receptors. Here we describe a new gene family in A. thaliana named prePIPs, whose members encode secreted peptide precursors, and show that one of its members, prePIP1, is secreted into extracellular space and cleaved at the C-terminus. Exogenous application of PIP1, the synthetic 13-amino acid peptide corresponding to the conserved C-terminal region of prePIP1, triggered immune responses and led to enhanced pathogen resistance in A. thaliana. We further provide evidence showing that PIP1 signals via the receptor-like kinase 7 (RLK7) and employs both shared and distinct components with the PEP1 signaling pathway. Both PIP1 and PEP1 cooperatively amplify the immune response triggered by flg22, the active epitope of bacterial flagellin.


Immune signaling in plants is typically initiated when immune-related receptors perceive the presence of pathogen molecules, including so-called “pathogen-associated molecular patterns” (PAMPs) and race-specific effectors [1]. PAMPs, such as bacterial flagellin and fungal chitin, are recognized by plasma membrane-located pattern recognition receptors (PRRs), which activate PAMP-triggered immunity (PTI). In addition, pathogen infection causes the release of endogenous damage-associated molecular patterns (DAMPs), such as peptides, oligogalacturonides (OGs), or cutin monomers. DAMPs are released from the cytoplasm or the cell wall into the extracellular space, where they induce immune responses resembling PTI following perception by PRRs [2][4]. Over a dozen PRRs have been identified. Most belong to the superfamily of receptor-like kinases (RLKs), characterized by an extracellular domain, a transmembrane region and a cytoplasmic kinase domain. Arabidopsis thaliana has more than 600 RLKs. Among these, the leucine-rich repeat RLKs (LRR-RLKs) constitute the largest group which has been divided into 13 categories (I through XIII) [5]. Flagellin-sensitive 2 (FLS2), a LRR-RLK from category XII, binds to a 22 residue epitope (flg22) present at the N terminus of flagellin from Gram-negative bacteria [6]. Perception of flg22 induces the dimerization and rapid phosphorylation of FLS2 and BRASSINOSTEROID INSENSITIVE 1-associated receptor kinase 1 (BAK1), as well as phosphorylation of the receptor-like cytoplasmic kinase (RLCKs) BIK1 [7][10]. The activated receptor complex triggers elevation of cytosolic calcium, generation of reactive oxygen species (ROS), phosphorylation of mitogen-activated protein kinases (MAPKs), callose deposition, and transcriptional reprogramming of the cell, leading to enhanced resistance against pathogens [11][14].

PEP1 was identified as an extracellular 23-aa peptide derived from the C-terminus of the A. thaliana precursor protein proPEP1. Since proPEP1 lacks an N-terminal signal peptide, the release of PEP1 into the apoplast was suggested to result from cellular damage caused by pathogen attack or wounding, suggesting that PEP1 functions as DAMP. Two XI category LRR-RLKs, PEPR1 and PEPR2, were shown to act as receptors of PEP1 and homologous peptides in A. thaliana [15], [16]. Perception of PEP1 by PEPR1/2 activates PTI and enhances host resistance against the pathogens Pseudomonas syringae and Pythium irregulare [3], [16]. PEPR1 also modulates ethylene (ET)-dependent resistance to Botrytis cinerea via the phosphorylation of BIK1 [17], [18]. Since expression of PEP1-PEPR1/2 is induced by flg22 and PEP1 itself, and since PEP1-PEPR1/2 employs shared components with PAMPs signaling, PEP1-PEPR1/2 has been proposed to function as an amplifier of PTI signaling [16], [19].

Secreted peptides coordinate a variety of plant developmental processes, including stem cell maintenance, stomatal development, lateral root initiation, vascular formation, floral abscission and cell expansion [20][22]. Recently, several secreted peptides have been reported to modulate plant immune signaling. For instance, the CLAVATA3 peptide (CLV3p), known to regulate stem cell homeostasis in the shoot apical meristem, was suggested to be recognized by FLS2 and activate FLS2-dependent immune responses in the shoot meristem [23]. The sulfated peptides phytosulfokine (PSK) and PSY1, were initially identified as promoters of cell proliferation and tissue growth, and were recently shown to attenuate PTI responses and to enhance susceptibility to biotrophic pathogen and resistance to necrotrophic pathogen [24], [25]. A. thaliana has been suggested to produce over 1000 secreted peptides [26], the overwhelming majority of which remain functionally uncharacterized. To look for secreted peptides potentially involved in regulation of immunity, we searched the available A. thaliana microarray data for flg22- and elf18-induced genes. This led to the identification of a novel gene family of secreted peptide precursors, termed “prePIPs” (precursors of PAMP-Induced Peptides). We provide evidence showing that PIP1 and PIP2, two peptides obtained from processing of the representative prePIP family members prePIP1 and prePIP2, are able to activate immune responses in A. thaliana and to enhance resistance against P. syringae and Fusarium oxysporum. Using a reverse genetics approach, we demonstrate that RLK7, a class XI LRR-RLK, is required for PIP1 and PIP2-elicited immune activation, and that PIP1-RLK7 has a crucial role in PTI amplification.


Screening of A. thaliana genes encoding PAMP-induced secreted peptide (PIP) precursors

Analysis of flg22- and elf18-induced transcription data (microarray accession number E-MEXP-547) resulted in the identification of 12 genes encoding putative secreted peptide precursors [27]. The predicted gene products were 70–110 amino acid residues in length and included an N terminal signal peptide, as predicted by the SignalP 3.0 server [28]. Of these, four have known or predicted functions. They include PSK4 precursor [29], PSY1 precursor [30], IDA [31], and an IDA-like protein (At1g05300). The other eight are functionally uncharacterized. Three of these eight genes (At4g28460, At4g37290, and At2g23270) share a highly conserved C terminus, and their products were named prePIP1, prePIP2 and prePIP3, respectively (Table S1). A blastp search based on the prePIP1 C terminus sequence revealed that A. thaliana has at least 11 prePIP homologs, including seven annotated and four non-annotated proteins. Orthologs of prePIP proteins are present in numerous species of dicots and monocots, such as soybean, grape, maize, and rice (Figure S1). All the prePIP family members exhibit the hallmarks of post-translationally modified secreted peptide precursors: a signal peptide at the N terminus, a highly conserved cysteine-poor region at the C-terminus (hereafter referred to as the SGPS motif), and a variable region between the signal peptide and the SGPS motif (Figure 1A) [20]. Eight A. thaliana family members contain a single SGPS motif while three (prePIP2, prePIP3 and prePIPL1) harbor two SGPS motifs. The prePIP SGPS motif shares structural features with CLV3/CLE peptides [32], [33], the IDA peptide (IDAp), CEP1 [34], and PEP1 [3]. Since all these peptides carry conserved Ser, Gly, Pro, and His residues (Figure S2), we propose that they form a superfamily called “SGP-rich” peptides.


During the process of translation, the prepropeptide, the original form of secreted peptide precursor, is targeted to the endoplasmic reticulum/Golgi-dependent secretory pathway where the N-terminal signal peptide is removed resulting in the propeptide. The propeptide is subsequently secreted into the apoplast and subjected to proteolytic processing, releasing the mature C-terminal peptide [20]. To experimentally determine whether the prePIP1 propeptide is secreted, the green fluorescent protein gene (GFP) was fused to the C-terminus of prePIP1 (prePIP1-GFP) under the control of the cauliflower mosaic virus 35S (CaMV 35S) promoter and transiently expressed in tobacco leaves using agro-infiltration. Confocal microscopy imaging showed that prePIP1-GFP fluorescence was distributed in the pericellular apoplastic space. In contrast, GFP protein alone was present in the cytoplasm and the nucleus. The secreted peptide precursor CLV3, which was previously shown to localize in the extracellular matrix, exhibited a similar localization as prePIP1-GFP when a C-terminal GFP fusion allele was expressed in tobacco leaves (Figure 1B). These results suggest that the prePIP1 product is secreted into the plant extracellular space.

An in-vitro assay was conducted to determine whether prePIP1 and prePIP2 are proteolytically processed. Glutathione S-transferase-tagged signal peptide-deleted prePIP1 and prePIP2 (GST-ΔP1 and GST-ΔP2) were expressed in E. coli strain BL21 (DE3) and purified through Glutathione Sepharose (Figure S3). Incubation of GST-ΔP1 and GST-ΔP2 in a reaction solution supplementing extracts of A. thaliana seedlings but not BSA (negative control) resulted in a reduction of 1–2 kDa in size (Figure 1C and D). When GST-ΔP1 was injected into A. thaliana leaves, a similar reduction in molecular size was detectable after a 2 h incubation, consistent with a cleavage of GST-ΔP1 by a plant protease(s) present in the extracellular space (Figure S4).

Expression of prePIP1

Transgenic plants carrying the GFP gene under control of the prePIP1 promoter exhibited strong fluorescence in guard cells, hydathodes and vascular tissue (Figure 2A). Interestingly, all these tissues represent either potential entry points or proliferation routes for invading pathogens. In contrast, no fluorescence was detected in these tissues in untransformed plants (data not shown). When A. thaliana seedlings were exposed to flg22 or chitin, prePIP1 transcription was markedly up-regulated (Figure 2B). Subsequent experiments, based either on transcript abundance or on the expression of a transgene carrying the β-glucuronidase (GUS) gene driven by the prePIP1 promoter, confirmed that prePIP1 was up-regulated during infection with the bacterial pathogen P. syringae DC3000 (Pst DC3000) or with the fungal pathogen F. oxysporum f. sp. conglutinans strain 699 (Foc 699) (Figure 2C). Transcript abundance increased about eight folds following inoculation with Pst DC3000 and about 15 folds with Foc 699, extending throughout the leaf and root system within 24 h after inoculation (Figure 2C–E). PrePIP1 expression was also increased in A. thaliana seedlings after treatment with immune-related phytohormones. Quantitative RT-PCR (RT-qPCR) analysis showed that the prePIP1 transcript was induced by methyl salicylate (MeSA), but not by methyl jasmonate (MeJA) or the ethylene precursor 1-aminocyclopropane-1-carboxylate (ACC). Importantly, expression of the SA pathway marker pathogenesis-related protein 1 (PR1) and of the JA pathway marker PDF1.2 was induced by MeSA and MeJA treatments, respectively (Figure 2F).


PIP1 and PIP2 inhibit A. thaliana root growth

A. thaliana transgenic lines overexpressing prePIP1 or prePIP2 (35S::prePIP1 and 35S::prePIP2) (Figure 3A) consistently exhibited a shorter main root than the wild type (WT) plants (Figure 3B and C). In contrast, transgenic plants overexpressing IDA and IDA-like were abnormal with respect to their floral abscission zone (AZ) [35]. In spite of the high sequence similarity between the C termini of IDA and prePIPs, overexpression of prePIP1 or prePIP2 did not affect AZ structure (Figure S5), indicating different functions of the two protein families.


Because post-translationally modified secreted peptides generally coincide with the C-terminal conserved region of their precursors [20], exogenous application of synthetic peptides such as CLV3p, IDAp, and CEP1 reproduces the phenotypes of overexpression lines of the respective precursor gene [32], [34], [35]. We tested whether addition of synthetic peptide PIP10 comprising the conserved SGPS-motif of prePIP1, could reproduce the effect on root growth of prePIP1 overexpression. PIP10 significantly inhibited the elongation of the main root when applied at a concentration of 100 nM (Figure 3D). Since SGP-rich peptides usually undergo proline hydroxylation, the inhibitory effect on root growth of three PIP1 derivatives, PIP1Hpy6, PIP1Hpy8, and PIP1Hpy6, 8 (Table S2) was investigated. Of these, PIP1Hyp6 (hereafter denoted “PIP1”) and PIP1Hpy6, 8 were more active than PIP10 (Figure 3D), suggesting that proline hydroxylation at position 6 contributes to biological activity of the peptide. PIP1 activity was also pH dependent, since root growth inhibition was most active in the pH range 5.8–6.8 (Figure 3E). Results for PIP2, the synthetic hydroxylated peptide corresponding to prePIP2, were similar to those obtained with PIP1 (Figure 3F).

PIP1 and PIP2 elicit immune responses in A. thaliana

The role of the peptide derived from prePIP1 in plant immunity was explored initially using a transient expression assay in mesophyll protoplasts. The firefly luciferase gene (LUC) driven by the promoter of Flg22-induced Receptor-like Kinase 1 (FRK1), a marker gene of PTI signaling, was co-transfected as a reporter with either prePIP1, prePIP1ΔSP (prePIP1 lacking the signal peptide), or prePIP1ΔSGPS (prePIP1 lacking the SGPS-motif) all driven by the CaMV 35S promoter. Activation of the FRK1 promoter was only detected with a full length copy of prePIP1, implying that both secretion of prePIP1 and its SGPS-motif are required for FRK1 induction (Figure 4A and B). Similar to flg22 and PEP1, exogenous application of PIP1 and PIP2 induced the expression of pFRK1::LUC in protoplasts, but neither IDL2 nor CEP1 did (Figure 4C). Moreover, RT-PCR and RT-qPCR analyses revealed that PIP1 and PIP2 induced transcription of the immune response genes FRK1, WRKY30, WRKY33, WRKY53, and PR1 (Figure 5A–C and S6). Other characteristic PTI responses such as stomatal closure (Figure 5D), ROS production (Figure 5E), callose deposition (Figure 5F), and MAPK phosphorylation (Figure 5G) were also induced by these two peptides. In comparison with flg22, PIP1, PIP2 and PEP1 induced significantly lower ROS production and leaf callose deposition (Figure 5E and F). Similarly, the effect of PIP-induced immunity on host resistance against Pst DC3000 was weaker than that induced by flg22. Treatment with 1 µM PIP1 or PIP2 delayed Pst DC3000 proliferation in leaves by ∼70%, while 1 µM flg22 decreased bacterial growth by >90% (Figure 5H).



The prePIP1 gene is abundantly expressed in A. thaliana roots. We therefore measured PIP-induced immunity in roots using a MYB51p::GUS reporter which was previously employed to monitor flg22-triggerred immune responses [36]. PIP1, PIP2, PEP1 and flg22 strongly activated MYB51 promoter activity in the root elongation zone (EZ) (Figure 6A). MYB51-dependent indole-glucosinolate synthesis is required for callose deposition [37]. All peptides induced callose deposition in the root EZ (Figure 6A), while no such induction was detectable in the presence of CEP1 or IDL2 (Figure S7).


Given that prePIP1 expression was induced upon Foc 699 infection, resistance against this pathogen was compared between WT and 35S::prePIP1 or 35S::prePIP2 plants. When A. thaliana seedlings were challenged with microconidia of GFP-labeled Foc 699 (Foc 699-GFP), fungal hyphae penetrated the EZ cortex 3–6 h post infection and reached the vascular tissue ∼12 hours later (Figure S8). However, the extent of Foc 699 penetration in the roots of 35S::prePIP1 and 35S::prePIP2 plants was significantly lower than in the roots of WT, as estimated from the GFP fluorescence signal (Figure 6B and C). When Foc 699 infected seedlings were potted into soil and left to grow for three weeks, the overexpression lines displayed a significantly reduced mortality compared to the WT plants (Figure 6D). These results indicate that overexpression of prePIP1 or prePIP2 enhances Arabidopsis resistance against Foc 699.

RLK7 is the PIP1 receptor

Secreted peptides are typically recognized by plasma-localized LRR-RLKs [21]. The sequence similarity between PIPs and other SGP-rich peptides suggested that the hypothetical PIP1 receptor(s) could be structurally related to the CLV3p receptor CLV1 [38], the IDAp receptors HAE and HSL2 [35], or the PEP1 receptors PEPR1/2 [15], [16], all of which are class XI LRR-RLKs [5]. Like PEPR1/2 and other immune-related receptors, the hypothetical PIP1 receptor(s) is likely to be up-regulated by pathogen attack or PAMP induction. The A. thaliana genome harbors 28 category XI LRR-RLKs genes, six of which are induced by PAMP treatment or pathogen infection [27], [ 39]: PEPR1/2, HAE, RLK7 (At1g09970), At5g25930 (here named HSL3), and SOBIR1. The SOBIR1 product was shown to act as a co-regulator of multiple receptor-like proteins (RLPs) that are involved in immune recognition [40][42], and was suggested not to function directly in ligand recognition due to its short LRR domain. To identify the putative receptors of PIP1 and PIP2, we analyzed the response of T-DNA insertion mutants of RLK7, HAE, HSL2, HSL3, and FLS2 to PIP1 and PIP2 treatments. No inhibition of root growth was observed in two rlk7 mutants, rlk7-2 and rlk7-3, while the other mutants responded similar as the WT (Figures 7A, S9). The roots of 35S::prePIP1 or 35S::prePIP2 plants were significantly shorter than those of WT plants, while roots of the double homozygous F2 progeny of a cross between 35S::prePIP1 or 35S::prePIP2 and rlk7-3 grew normally as did those of rlk7 mutants. Thus, inhibition of root growth by prePIP1 and prePIP2 is RLK7 dependent (Figure 7B).


In contrast to the WT, the rlk7-3 plants failed to up-regulate expression of FRK1, WRKY33, and WRKY53 upon treatment with PIP1 or PIP2 (Figure 7C and S10A and B). In contrast, flg22 strongly induced expression of FRK1 both in WT and rlk7-3 plants, but not in the fls2 mutant (Figure S10C), suggesting that RLK7 responds specifically to PIPs. Moreover, PIP1-induced MPK3 and MPK6 phosphorylation was also abolished in rlk7-3 (Figure 7D), as was the increase of host resistance against Pst DC3000 infection by pre-treatment of Arabidopsis leaves with PIP1 (Figure 7E). The prePIP1 overexpression line displayed a significantly reduced mortality compared to the WT plants as indicated above, while the double homozygous F2 progeny of a cross between 35S::prePIP1 and rlk7-3 displayed a higher mortality as did those of rlk7-3 mutants (Figure 7F).

We next asked whether RLK7 directly binds the PIP1 peptide. This was first addressed through a pull-down assay with biotinylated PIP1 in A. thaliana plants expressing hemagglutinin (HA) tagged-RLK7 (RLK7-HA). Two derivatives of biotin labeled PIP1 (Biotin-PIP1 and PIP1-biotin) were confirmed to maintain their biological function by determining their activities on root growth inhibition and marker gene induction (Figure S11). Since PIP1-biotin exhibited a higher activity, it was used for all subsequent experiments. We found that RLK7-HA was pulled down with PIP1-biotin-associated streptavidin beads from membrane protein extracts of rlk7-3 plants harboring RLK7-HA, but not from rlk7-3 plants (Figure 7G). Binding of RLK7-HA to the beads was inhibited by a 100× excess of unlabelled PIP1 but not by unlabelled IDA. Next, a chemical cross-linking assay was employed to prove a direct binding of PIP1-biotin to RLK7-HA. PIP1-biotin peptide was incubated with protein extracts of RLK7-HA transgenic plants or rlk7-3 mutants, and cross-linked with its potential receptor using a chemical cross-linker. After separation by SDS-PAGE, protein samples were hybridized with an anti-biotin antibody. A protein of 130 kD, consistent with the molecular mass of RLK7-HA, was detected in RLK7-HA plants but not in rlk7-3 mutants (Figure 7H), suggesting that the protein corresponds to the RLK7-HA protein. Binding of PIP1 to RLK7 was further corroborated using a photoaffinity labeling assay. RLK7-HA or GFP (negative control) were transiently expressed in tobacco leaves, and homogenized leaf tissues were incubated with 1 nM 125I-labeled PIP1 in the presence or absence of 10 µM unlabeled PIP1. Specific binding of 125I-labeled PIP1 was detected in the homogenate from leaves expressing RLK7-HA protein, but not in those from leaves expressing GFP (Figure 7I).

PIP1-RLK7 signaling is partially dependent on BAK1, but independent of BIK1

The receptor kinase BAK1 plays an important role in PTI immune activation by forming heteromeric co-receptor complexes with multiple LRR-RLK receptors, including FLS2 and PEPR1 [7], [8], [39]. Sensitivity to flg22 and PEP1 was partially reduced in bak1 T-DNA insertion mutants bak1-3 and bak1-4 [43]. While dimerization of FLS2 with BAK1 occurs after flg22 perception by FLS2, PEPR1 interacts constitutively with the kinase domain of BAK1. Since PIP1 triggers similar early immune responses as flg22 and PEP1, we asked whether BAK1 also contributes to PIP1 responses. Indeed, PIP1-induced ROS production and root growth inhibition were both reduced in bak1-4 than in WT plants (Figure 8A and B). In contrast, while PEP1-induced ROS production was also reduced in the bak1-4 mutant, inhibition of root growth was unaffected (Figure 8A and B). Thus, while PIP1-RLK7 signaling is partially dependent on BAK1, PIP1 and PEP1-induced responses have different requirements for BAK1.


FLS2 and PEPR1 initiate downstream signaling by directly interacting with the receptor-like cytoplasmic kinase BIK1 [9], [17]. Therefore, we investigated the possible interaction between BIK1 and RLK7. Yeast two-hybrid results did not indicate an interaction between BIK1 and the kinase domain of RLK7, while confirming the interaction between BIK1 and the kinase domain of PEPR1 reported previously (Figure 9A). In plants lacking BIK1, flg22- and PEP1-induced root growth inhibition was attenuated while the effect of PIP1 was unchanged (Figure 9B). Given the known role of PEPR1-BIK1 in mediating ET responses [17], we compared hypocotyl elongation in WT and rlk7 seedlings treated with ACC, but found no significant difference (Figure 9C and D). However, sensitivity to ACC treatment was attenuated in both ein2 (ethylene insensitive 2) and bik1 mutants. Taken together, these results suggest that PIP1-RLK7 signaling is independent of BIK1.


PIP1-RLK7 and PEP1-PEPR1 cooperate to amplify FLS2 signaling

Because the expression of prePIP1 and RLK7 is induced by flg22 and PIP1 triggers a similar immune response to flg22, we hypothesized that PIP1-RLK7, like PEP1-PEPR1, may serve to amplify PAMP signaling. In support of this idea, flg22- or chitin-induced callose deposition was more pronounced in leaves and roots of 35S::prePIP1 or 35S::prePIP2 plants than in WT plants (Figure 10A–C). Moreover, we observed an additive effect in elevation of host resistance against Pst DC3000 in plants pre-treated simultaneously with flg22 and PIP1, compared to each single peptide elicitor (Figure 10D). Furthermore, activation of WRKY33 and PR1, two genes representing, respectively, early- and late-response immune reporters, by flg22 was reduced in rlk7 plants compared to WT plants (Figure 10E and F), and the level of flg22-induced host resistance against Pst DC3118 (a coronatine deficient Pst DC3000 mutant) was less marked in the rlk7 mutant (Figure 10G). Finally, PIP1 and PEP1 both appeared to enhance flg22 responses via up-regulation of FLS2 expression (Figure 10H).


A crosstalk between PIP1 and PEP1 signaling was further supported by the finding that PEP1-induced root growth inhibition and WRKY33 expression were impaired in mutants lacking RLK7 (Figure S12). Either PEP1 or PIP1 induced the transcription of all the genes encoding precursors and receptors of the two peptides (Figure 10I–L). Thus, PIP1-RLK7 and PEP1-PEPR1 act cooperatively to amplify FLS2-initiated immunity.


PIP1 is a functional secreted peptide

The identification of elicitors to date has relied on various bioassays conducted on extracts of pathogen and/or host tissue [3], [44], [45]. Because the active components are typically present in low abundance, this mode of analysis is technically challenging. With the widespread development of genomic and transcriptomic data in A. thaliana, bioinformatics is increasingly offering potential for predicting the identity of elicitors. Here, by analyzing PAMP-induced gene transcription data, a gene family encoding precursors of the secreted peptide elicitors PIPs was identified.

The release from precursor proteins by proteolysis in the extracellular space is a critical process for secreted peptides [20]. In vitro, prePIPs are typically cleaved close to the C terminus. Specific cleavage was confirmed in vivo, since recombinant GST-ΔP1 protein suffered a similar processing pattern when injected into leaves of A. thaliana. Although it is generally assumed that mature peptides are released from precursors through endopeptidase-mediated cleavage [46], the only cleavage recognition site identified so far in A. thaliana is a specific sequence in the peptide PSK4 which was confirmed to be proteolytically cleaved by the subtilase SBT1.1 [46]. In most post-translationally modified secreted peptide precursors, cleavage occurs before or after Arg, Asp, His or Asn residues located at both sites of the C-terminal conserved motifs [20]. Members of the prePIP1 family harbor a conserved Arg or His residue at each side of the SGPS-motif. We found that exogenous application of synthetic PIP1 peptide corresponding to the conserved SGPS-motif successfully mimicked the phenotypes of A. thaliana plants transiently or constitutively expressing prePIP1. This indicates that PIP1 is a biologically active form derived from prePIP1, and shares part or all of the sequence with the genuine mature peptide cleaved from the precursor. However, considering that PIP1 peptide was saturated at micromolar concentration in root growth inhibition assays, we cannot exclude the presence of a more active peptide. Further, a mass spectrometry analysis is needed to confirm the cleavage site and to identify the mature peptides cleaved from prePIPs precursors.

Proline hydroxylation is common in SGP-rich peptides such as CLV3p and CEP1 [33], [34]. PIP family members harbor two conserved proline residues. A comparison of the root growth inhibitory effect of proline hydroxylated and non-hydroxylated forms of PIP1 revealed that hydroxylation enhances the biological activity of the peptide. In contrast, unmodified CLV3 and hydroxylated CLV3 peptides had similar activities in root growth inhibition [32], [33]. This suggests that proline hydroxylation differentially affects the biological activities of PIP1 and CLV3. It is currently not clear whether proline hydroxylation of PIP1 affects its affinity for the receptor or its stability.

PIP1 activates plant immunity in an RLK7-dependent manner

We found that the PIP1 and PIP2 peptides activate similar immune responses as flg22 and PEP1, including expression of marker genes, ROS production, callose deposition and MAPK activation. The possibility that this result was caused by contamination with flg22 and/or PEP1 can be excluded for several reasons. First, independently synthesized PIP peptides exhibited the same activity; second, IDL2p and CEP1, two peptides with a similar sequence structure to PIPs that were synthesized together with PIPs, failed to activate immune responses; third, a fls2 loss-of-function mutant that is insensitive to flg22 still responded to PIPs; and fourth, PIP1 and PEP1 differed functionally from each another.

A reverse genetics screen identified the class XI LRR-RLK RLK7 as the responsible for PIP1- and PIP2-triggered responses. RLK7-PIP1 binding data implicate that RLK7 acts as the PIP1 receptor. However, the flg22 receptor FLS2 which was previously proposed to perceive CLV3p and Ax21 [23], [47], [48], failed to recognize PIP1 since fls2 mutants were still responsive to PIP1-induced up-regulation of FRK1. Although RLK7 was required for the PIP1-induced enhancement of host resistance against Pst DC3000, loss-of-function rlk7 mutants showed no reduction in the level of resistance in the absence of PIP1 treatment. This is reminiscent of the finding that the pepr1/pepr2 double mutant is not affected in the level of resistance against Pst DC3000 [16]. The virulence of Pst DC3000 relies heavily on secreted effector proteins which can suppress host immunity by blocking various signaling pathways [49]. The resistance conferred by the PIP-RLK7 signaling pathway may thus be severely disrupted by pathogen effectors. Moreover, the expression pattern of prePIP1 suggests that PIP1-RLK7 resistance is perhaps more specific to pathogens infecting through the hydathodes or proliferating in the vascular tissue. This idea is consistent with the high host resistance conferred by prePIP1 or prePIP2 over-expression against the fungus Foc 699, a soil-borne pathogen that colonizes the root vascular tissue.

PIP1-RLK7 share overlapping but also distinct signaling components with PEP1-PEPR1

PIP1 activates an almost identical set of signaling events as flg22 and PEP1, suggesting that the three pathways likely share a number of components. BAK1 regulates several of the immune signaling pathways triggered by LRR-RLK type immune receptors, including FLS2 and PEPR1 [7], [8], [39]. We found that PIP1-RLK7 mediated responses are less pronounced in bak1-4 mutants, suggesting that BAK1 contributes to PIP1-RLK7 signaling. Previous studies suggested that BAK1 and BAK1-LIKE1 (BKK1) function in parallel in FLS2- and PEPR1-activated immune signaling, since the bak1 mutant is only partially insensitive to flg22 and PEP1 while the bak1/bkk1 double mutant is completely insensitive [7], [39], [43]. We noted that the bak1-4 mutant retained some sensitivity to PIP1, implying some degree of redundancy between BAK1 and BKK1. However, both flg22- and PIP1-induced ROS production and root growth inhibition were attenuated in the bak1-4 mutant, whereas only ROS production was affected upon induction with PEP1. This suggests possible differences in the requirement for BAK1 between flg22, PEP1 and PIP1 responses.

BIK1, another important regulator of the FLS2 and PEPR1 signaling pathways, is rapidly phosphorylated when flagellin binds to FLS2 [9]. BIK1 phosphorylation can also be induced with PEPR1 or PEPR2 in the presence of ET or PEP1 [17]. This is consistent with the results from our root growth inhibition assay and previous ET-induced triple response analysis. No direct protein-protein interaction between RLK7 and BIK1 could be detected by yeast two-hybrid analysis, and no parallels were found between PIP1-RLK7 and PEP-PEPR1 in the context of the ET response. Neither did the rlk7 mutants show reduced sensitivity to ACC, nor was PIP1-induced root growth inhibition attenuated in the bik1 mutant. BIK1 is a member of class VII RLCKs, which have been suggested to integrate immune signaling in A. thaliana from cell-surface-localized receptors [9], [10]. Thus it is possible that other members of class VII RLCKs mediate RLK7 signaling and are responsible for the observed differences in signaling outputs between RLK7 and PEPR1.

ProPEP1 family members lack a classical signal peptide, and therefore the mechanism underlying PEP release is unclear. Since expression of proPEP1 is up-regulated by wounding and treatment with the wound signal MeJA, it was suggested that release of PEP1 from plant cells may be the result of cell injury caused by pathogen attack or wounding [3]. Consistent with this, PEPR signaling was recently shown to operate predominantly at local pathogen challenged sites, though systemic immunity can be activated by treatment with PEP1 [50]. In contrast, PIP1 is secreted into the extracellular spaces through a cell-autonomous secretory pathway and massive expression of prePIP1 is detected in vascular tissues, suggesting that PIP1 is likely to act as a mobile signal involved in systemic immune activation.

PIP1-RLK7 and PEP1-PEPR1 cooperatively amplify FLS2 signaling

Activation of immunity by endogenous signals is a common strategy exploited by animals and plants to amplify immune responses after perceiving a limited number of invading pathogens [51]. In animals, many endogenous peptides such as interleukins which are generated upon PAMP recognition, were confirmed to function in inflammation [52]. In plants, PEP1 was suggested to act as a PTI amplifier because (1) PAMP treatment increases transcription of proPEP1, (2) PEP1 and PAMPs activate similar immune responses, and (3) PEP1 receptors are required for full activation of PTI signaling and resistance against bacterial infection [16], [18], [53]. In this study, prePIP1 and RLK7 were induced by flg22, and flg22-triggered immunity was impaired in rlk7 mutants. These findings imply that PIP1-RLK7 and PEP1-PEPR1 have similar functions in FLS2 signal amplification. PIP1 and PEP1, respectively, induce their corresponding precursor and receptor genes showing that self-amplification mechanisms act in both signaling pathways. Importantly, PIP1 and PEP1 also induce the expression of each other's precursor and receptor genes. Further, the level of PEP1 responses was decreased in rlk7 mutants. These demonstrate that the two endogenous peptide signaling pathways are interdependent and cooperate to amplify the immune response. We propose a working model (Figure 11) in which FLS2 signaling is initially primed by the perception of flg22, followed by upregulation of the host peptide elicitors PIP1 and PEP1 and their respective receptors PEPR1 and RLK7. Once PIP1 and PEP1 are released and processed in the apoplast, they initiate the immune response and also increase expression of prePIP1, RLK7, proPEP1, PEPR1 and FLS2, leading to an amplification of the immune responses via the combined effect of FLS2, PEPR1 and RLK7.


Materials and Methods

Plant materials

A. thaliana were grown in potting mix or on 1/2 MS medium (containing 1/2 MS salts, 1% w/v sucrose and 0.8% w/v agar, pH 5.7) in a controlled growth chamber providing a 10 h photoperiod (140 µmol•m−2•s−1 light) at 22°C/20°C day/night and 60% relative humidity. fls2 [54], rlk7 [55], hae/hsl2 [35], ein2-1 [17], bak1-4 [7], and bik1 [10] mutants used were described earlier. Verification of homozygous T-DNA insertion mutants was carried out by a PCR assay based on locus-specific primers (Table S3).

Root growth inhibition assay

Arabidopsis seedlings were germinated on 1/2 MS media, and then transferred to 1/2 MS liquid medium (1/2 MS salts, 1% sucrose, pH 5.7) adding various concentrations of PIP1 or other peptides in a 6-well plate. The length of the seedling roots was measured after 5–7 days.


PrePIP1, prePIP2, and RLK7 coding sequences were PCR-amplified from A. thaliana genomic DNA using locus-specific primers, and the products were separately inserted into pCAMBIA1300-HA vector downstream of the CaMV 35S promoter to generate pCAMBIA1300-35S::prePIP1-HA, pCAMBIA1300-35S::prePIP2-HA and pCAMBIA1300-35S::RLK7-HA. An ∼2.8 kb fragment upstream of the prePIP1 start codon was amplified from A. thaliana genomic DNA and inserted into the pGFPGUSPlus vector [56] to construct prePIP1p::GUS and prePIP1p::GFP. Truncated prePIP1, prePIP2 and prePIPL5 coding sequences were amplified from A. thaliana genomic DNA using locus-specific primers and inserted into pGEX-6p-1 to generate GST-ΔprePIP1, GST-ΔprePIP2, GST-ΔprePIPL5. The BIK1 coding sequence was amplified from A. thaliana cDNA and inserted into pGBKT7 to generate pGADT7-BIK1. The sequences encoding the kinase domains of PEPR1 (residues 827–1123) and RLK7 (residues 671–977) were amplified from A. thaliana cDNA and inserted into pGADT7 to generate pGADT7-PEPR1KD and pGADT7-RLK7KD. All the sequences primers are listed in Table S3.

Synthetic peptides

Peptides of purity level 98% were synthesized by Yaguang Biochemical Company (Shanghai, China). Their sequences are given in Table S2.

Transient expression in tobacco leaves

Transient expression in tobacco leaves was performed as described previously [57]. Agrobacterium tumefaciens strain GV3101 harboring pCAMBIA1300-RLK7-HA, pCAMBIA1300-GFP, pCAMBIA1300-prePIP1-GFP or pCAMBIA1300-CLV3-GFP were grown overnight in YEB medium and transferred to 1/2 MS liquid medium containing 50 µM acetosyringone for 4 h until an OD600 of 0.4–0.6 had been reached. The culture was then diluted 1∶1 with 10 mM MES (pH 5.6), 10 mM MgCl2, 150 µM acetosyringone, and pressure-infiltrated into the leaves of 4–5 week old tobacco plants. Transfected leaves were collected after 48–72 h.

Proteolytic processing assays

In-vitro cleavage assays were performed as described previously [58]. In brief, GST-tagged truncated prePIPs (GST-ΔPIPs) were expressed in E. coli BL21 (DE3) and purified using glutathione Sepharose (GE Healthcare). The purified proteins were incubated with Arabidopsis protein extracts or BSA (control) for 0–2 h at room temperature. The samples were then subjected to SDS-PAGE to determine the protein composition. For the in-vivo cleavage assay, GST-PIP1 (1 µg/µL) or GST (1 µg/µL) was syringe-injected into A. thaliana leaves and incubated for 2 h, then extracellular fluids were extracted and analyzed by SDS-PAGE.

GUS staining

GUS staining was performed as described previously [36]. In brief, plant tissues were immersed in staining buffer (100 mM sodium phosphate buffer, pH 7.0, 10 mM EDTA, 1 mM potassium ferrocyanide, 1 mM potassium ferricyanide, 1 mM X-Gluc, and 0.1% Triton X-100) and incubated at 37°C for 2–6 h. Stained samples were cleared in 70% ethanol and observed by the Olympus BX53 microscope.

Luciferase reporter assay

Protoplast transfection and subsequent luciferase reporter assay were performed as described previously [14]. FRK1p-LUC reporter was co-transfected with prePIP1 constructs and UBQ10p-GUS (internal control). After 6 hours' incubation, luciferase activities were tested with a Luciferase Assay kit and a GloMax-20/20 luminometer (Promega). For analysis of FRK1p-LUC induction by exogenous application of peptide elicitors, protoplasts were incubated overnight after transfection with FRK1p-LUC reporter, and then were induced with 1 µM peptide for 4 hours before detection of luciferase activity.

Quantitative RT-PCR analysis

Total RNA was extracted from plant tissues by the TRIzol reagent (Invitrogen) following the manufacturer's protocol. A 2 µL aliquot of the total RNA preparation was subjected to reverse transcription using a RevertAi First Strand cDNA Synthesis kit (Fermentas). The resulting cDNA was amplified using the SYBR Green Mix (Roche) and gene-specific primers (Table S3). AtActin2 was used as the reference sequence.

ROS measurement

A luminol-based assay was used to quantify ROS in treated leaves [59]. The same amount of 1–2 mm leaf fragments cut from Arabidopsis leaves were incubated in 100 µL water for 12 h, and then 100 µM luminol (Sigma), 10 µg/mL horseradish peroxidase (Sigma) and 1 µM peptide were added rapidly in turn. The resulting luminescence was measured using a GloMax-20/20 luminometer (Promega) at one minute intervals over 15 min.

Aniline blue staining

Staining of callose deposits was achieved following methods described previously [36], [59]. Adult leaves were infiltrated with either water or 1 µM peptide for 8 h, and the roots of 10-day old seedlings were immersed in 1/2MS liquid medium with or without peptides (1 µM) or chitin (500 µg/L) for 18 h. The materials were then fixed in 3∶1 ethanol∶acetic acid for 6 h, changing the fixative solution every 2 h. The samples were rehydrated in 50% ethanol for 2 h, and then thoroughly rinsed in water. Finally the samples were incubated in staining solution (150 mM K2HPO4 (pH 9.5), 0.01% (w/v) aniline blue, Sigma-Aldrich) for 30 min. Callose was visualized using UV-epifluorescence microscopy. Signal intensities were estimated using Image J software.

MAPK assay

Ten seedlings were immersed in sterile water overnight. Peptides were then added to a final concentration of 1 µM for 5–15 minutes induction. After induction, the seedlings were snap-frozen in liquid nitrogen and ground to a fine powder, from which total protein was extracted by suspension in 50 mM HEPES (pH 6.8), 150 mM NaCl, 1% (w/v) SDS, 2 mM DTT, 10 mM NaF, 10 mM NaVO3, 5 mM EDTA, 1× protease inhibitor cocktail (Roche). An anti-phospho p44/p42 MAPK antibody (Cell Signaling Technology) was used to detect active MPK6 and MPK3 via immunoblotting.

Binding assay

Y-PIP1 peptide was labeled with 125I as described previously [60]. In brief, 2 nmol Y-PIP1 peptide and 600 µCi Na125I (PerkinElmer) dissolved in 100 µL sodium phosphate buffer (10 mM, pH 7.4) were added into a glass vial pre-coated with 1,3,4,6-tetrachloro-3α,6α-diphenylglycouril, and were incubated for 15 min at root temperature. After passing through a Sephadex G25 column (PD-10 column, GE Healthcare), ∼800 µL 125I-Y-PIP1 containing 1.7×107 counts per minute (cpm) was collected. Plasma membrane fragments were extracted from 200 mg tobacco leaves and re-suspended in binding buffer (25 mM MES, pH 6.0, 3 mM MgCl2, 10 mM NaCl, 2 mM dithiothreitol and protease inhibitor cocktail (Roche)) with a final concentration of 2 µg/µL total protein. The plasma membrane (100 µL) was incubated with 2 µL 125I-Y-PIP1 (∼100 fmol) in the presence or absence of 10 µM unlabelled PIP1 for 15 min at 4°C, then were collected by a vacuum filtration system through glass fibre filters (Millipore, 2.5-cm diameter). After washed with cold washing buffer (binding buffer supplemented with 1% BSA, 1% bactotrypton, 1% bactopepton), the binding was determined by γ-counting.

Biotinylated-PIP1 pull-down assay

Plasma membrane proteins were extracted from the Arabidopsis leaves of rlk7 mutant and rlk7/35S::RLK7-HA with an extraction buffer (25 mM MES/KOH (pH 6.0), 3 mM MgCl2, 10 mM NaCl, 0.5% SDS and 1× protein inhibitor cocktail (Roche)), then were diluted ten folds with a binding buffer (25 mM MES/KOH (pH 6.0), 3 mM MgCl2, 10 mM NaCl and 1× protein inhibitor cocktail (Roche)). Biotinylated PIP1 (1 µg) was coupled to 20 µL streptavidin beads (Pierce) for 1 h at 4°C. After three rinses in 500 µL binding buffer, the beads were incubated with 200 µL of the prepared plasma membrane proteins in the presence or absence of 100× excess of unlabelled PIP1 or IDA for 2 h at 4°C. After rinsed three times in 500 µL binding buffer, the beads were boiled for 5 minutes in 50 µL 1× Laemilli buffer. The RLK7-HA was detected with an anti-HA monoclonal antibody (Qiagen).

Chemical cross-linking

Chemical cross-linking of PIP1-biotin to RLK7 was displayed as described previously. PIP1-biotin (1 µM) was incubated with the total protein (50 µg) extracted from rlk7 or 355S::RLK7-HA plants in the presence or absence of excess (50 µM) unlabeled PIP1 for 30 min at 4°C. After adding 1/10 volume of 25 mM EGS (Pierce), the mixture was incubated for another 30 minutes at room temperature before the reaction was terminated by the addition of 1 µL Tris-HCl buffer (1 M, pH 7.5). Proteins in samples were separated by SDS-PAGE and detected with anti-biotin antibody (Cell Signaling Technology).

Yeast two-hybrid assay

Interactions between BIK1 and the kinase domain of PEPR1 (residues 827–1123) or RLK7 (671–977) were tested using the GAL4 yeast two-hybrid system (Clontech). In brief, the pGADT7-PEPR1KD or pGADT7-RLK7KD plasmid was co-transfected with pGBKT7-BIK1 into Saccharomyces cerevisiae strain AH109. The transformed yeast cells were spotted on a synthetic dropout (SD) medium (Difco Yeast Nitrogen Base) lacking tryptophan, leucine, and histidine (SD-Y-L-H) but supplementing with 3 mM 3-amino-1,2,4-triazole (3-AT, Sigma) to detect the His reporter activity. Transformants were also detected on the basis of lacZ reporter activity with 50 µg/mL X-gal dissolved in 25 mM phosphate buffer.

Pathogen inoculations and quantification

Pst DC3000 inoculation assay was performed as described previously [61]. The bacterial suspension (2×105 colony-forming units (cfu)/mL) with or without 1 µM peptide was syringe infiltrated into leaves of 5-week old A. thaliana plants. Foc 699-GFP strain was obtained by cotransformation of the F. oxysporum f. sp. conglutinans strain 699 with the sGFP coding region driven the Aspergillus nidulans gpdA promoter and the trpC terminator, and the hygromycin resistance cassette, as described previously [62], [63]. Foc 699-GFP was grown in half strength potato dextrose broth at 28°C for 2 to 3 days. Ten day old seedlings were exposed to a 2 mL volume of a microconidia suspension (1×106 spores/mL sterile water) and incubated for 3–24 h at 22°C. To quantify Foc 699-GFP biomass, genomic DNA was extracted from 30 infected seedlings after rinsing them three times in sterile water, and used as a template for qPCR with GFP-specific primers (Table S3). The AtActin2 gene was used as the reference sequence. To monitor infection, Arabidopsis seedlings were rinsed three times with sterile water after 6-hour incubation with spore solution, planted into soil, and survival of the plants was assessed after 21 days.

Accession numbers

Sequence information of genes involved in this article can be found in the Arabidopsis information resource or the Arabidopsis unannotated secreted peptide database under the following accession numbers: At4g28460 (prePIP1), At4g37290 (prePIP2), At2g23270 (prePIP3), At1g49800 (prePIPL1), At3g06090 (prePIPL2), At4g37295 (prePIPL3), At5g43066 (prePIPL4), ath_mu_ch1_43150top (prePIPL5), ath_mu_ch5_43674top (prePIPL6), ath_mu_ch4_17161top (prePIPL7), ath_mu_ch5_43661top (prePIPL8), At1g09970 (RLK7), At5g46330 (FLS2), At1g73080 (PEPR1), At1g17750 (PEPR2), At2g31880 (SOBIR1), At4g28490 (HAESA), At5g65710 (HSL2), At5g25930 (HSL3), At5g64900 (proPEP1), At4g33430 (BAK1), At2g39660 (BIK1), At5g24110 (WRKY30), At2g38470 (WRKY33), At4g23810 (WRKY53), At2g19190 (FRK1), At2g14610 (PR1), At5g44420 (PDF1.2), At1g18570 (MYB51), At5g03280 (EIN2), At1g68765 (IDA), At5g64667 (IDL2), At1g47485 (CEP1).

Supporting Information


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