Lignin, one of the most abundant biopolymers on Earth, derives from the plant phenolic metabolism. It appeared upon terrestrialization and is thought critical for plant colonization of land. Early diverging land plants do not form lignin, but already have elements of its biosynthetic machinery. Here we delete in a moss the P450 oxygenase that defines the entry point in angiosperm lignin metabolism, and find that its pre-lignin pathway is essential for development. This pathway does not involve biochemical regulation via shikimate coupling, but instead is coupled with ascorbate catabolism, and controls the synthesis of the moss cuticle, which prevents desiccation and organ fusion. These cuticles share common features with lignin, cutin and suberin, and may represent the extant representative of a common ancestor. Our results demonstrate a critical role for the ancestral phenolic metabolism in moss erect growth and cuticle permeability, consistent with importance in plant adaptation to terrestrial conditions.
Land plants evolved from charophycean freshwater green algae around 450 Ma (refs 1, 2). Key challenges associated with terrestrialization would have included increased biomechanical stresses, desiccation, rapid temperature fluctuations and higher light intensity, particularly in the ultraviolet range. Colonization of land would therefore have required major metabolic adaptations in the form of ultraviolet screens, antioxidants and precursors for structural biopolymers to resist desiccation but to allow gas exchange between the plant and the environment to ensure proper photosynthesis. Three types of complex hydrophobic extracellular biopolymers are generally described as contributing to permeability control and water transport in the vegetative tissues of vascular plants, the evolution of which was likely guided by similar selective pressures: cutin, a lipid-derived component of the cuticle on aerial plant surfaces; suberin, which results from co-polymerization of lipid and phenolic derivatives and which regulates water movement in roots; and lignin, which is synthesized from phenolic precursors via the phenylpropanoid pathway and which reinforces secondary cell walls to enhance long-distance water transport and erect growth3,4,5. The metabolism of phenolic compounds was therefore likely a critical innovation for land colonization and, subsequently, the evolution and radiation of vascular plants through the development of lignified tissues6,7. Lignin-like polymers were recently identified in algae8,9, and phenylalanine/tyrosine ammonia lyases able to perform the first deamination step required for the synthesis of lignin precursors (that is, monolignols) from aromatic amino acids are present in algae and microorganisms10. However, orthologs of the next enzymes reported to frame the phenolic pathway in seed plants have not been found in algae, although they are present in bryophytes (mosses, liverworts and hornworts), the extant relatives of the earliest diverging land plants6,11,12, which played a major role in Earth’s oxygenation13. Mosses do not have true vasculature and are considered to be non-lignified plants14, but current perspectives suggest the possibility of a pre-lignin pathway arising in early non-vascular plants during the first stages of the transition from water to land3.
To address this idea, we investigated the function of a moss cytochrome P450 enzyme, in the CYP98 family, the homologue of which in flowering plants (angiosperms) catalyses the first irreversible step committed to the biosynthesis of the major monolignols. CYP98 enzymes from angiosperms catalyse the meta-hydroxylation of the phenolic ring of the phenylpropane C5-C3 unit of p-coumaric acid15,16,17 (Fig. 1). The substrate for this meta-hydroxylation reaction, resulting in the formation of a caffeoyl derivative, is not free p-coumaric acid, but an ester of shikimic acid17,18. This implies a coupling, in angiosperms, of monolignols production to the plastidial shikimate pathway that forms aromatic amino acids19. CYP98 inactivation in the model angiosperm Arabidopsis thaliana results in a severe suppression of growth and fertility16,20.
We show here that deletion of the single copy of CYP98 present in the genome of the model moss Physcomitrella patens prevents the moss gametophore development and cuticle formation. Our phenolic profiling indicates that the moss pre-lignin pathway mainly leads to the formation of soluble caffeoyl-threonic acids, whereas free caffeic acid or other caffeic acid conjugates cannot be detected. Accordingly, PpCYP98 catalyses the formation of caffeoyl-threonic acids in vitro. We show that the cuticle impermeability is strongly decreased in the ΔPpCYP98 mutants and can be restored together with plant growth by addition of caffeic acid. Our results thus demonstrate an essential role of the moss ancestral phenolic metabolism for plant erect growth and cuticle impermeability. These results are consistent with its proposed importance in plants terrestrialization.
PpCYP98 expression in developing gametophore and sporophyte
A single-copy CYP98 gene is present in the genome6 of the moss P. patens (PpCYP98; CYP98A34; Pp3c22_19010V3.1). Based on a transcriptome atlas21, the PpCYP98 gene is mostly expressed in above-ground haploid gametophytic and diploid sporophytic tissues (Supplementary Fig. 1). An assessment of the pattern of expression of PpCYP98 as determined after insertion of the uidA reporter gene encoding a β-glucuronidase (GUS) protein downstream of the PpCYP98 gene in transgenic moss lines (Supplementary Fig. 2) confirmed the transcriptome data, and revealed prominent expression in erect aerial organs (Fig. 2a–d; Supplementary Fig. 2). The highest PpCYP98 expression was observed in developing gametophores (Fig. 2a–c) and newly emerged and elongating phyllids (leaf-like structures; Fig. 2d), reproductive organs (gametangia: male antheridia and female archegonia), embryos and developing sporophytes including immature spores (Supplementary Fig. 2). Low levels of expression were also detected in the haploid filamentous protonema growing in direct contact with the wet substrate (Fig. 1b; Supplementary Fig. 1).
PpCYP98 prevents organ fusion
Three independent ΔPpCYP98 deletion lines were generated (Supplementary Fig. 3) and showed no evidence of altered growth of the protonema filaments (Fig. 2e,f; Supplementary Fig. 4), but consistently exhibited aborted gametophore formation, associated with evidence of organ fusion, thereby precluded from forming gametangia and from sexual reproduction (Fig. 2g–j). Similar phenotypes have been observed in mutants of seed plants that are impaired in biosynthesis of the lipid biopolymer, cutin22,23.
PpCYP98 controls the formation of caffeoyl-threonic acids
Comparing profiles of soluble phenolic compounds extracted from the gametophores, we observed a complete absence in the mutant of several major compounds present in the wild type (WT; Fig. 3a). Based on mass and induced fragmentation patterns, the missing compounds were identified as isomers of caffeoyl-threonic acid (Fig. 3b; Supplementary Fig. 5, Supplementary Table 1). Other major phenolic compounds with slightly altered abundances in the mutant were subsequently assigned p-coumaroyl-threonate structures (Fig. 3b; Supplementary Fig. 6, Supplementary Table 1). This suggested that p-coumaroyl-threonic acid might undergo CYP98-dependent meta-hydroxylation in moss. To test this hypothesis, the enzyme was expressed in yeast (Supplementary Fig. 7) and was shown to convert chemically synthesized p-coumaroyl-2-threonic and p-coumaroyl-4-threonic acid substrates (Supplementary Note 2) into caffeoyl-2-threonic and caffeoyl-4-threonic acids, respectively (Fig. 3c).
Neither caffeic acid nor caffeoyl-shikimate/quinate was detected in moss crude extracts (Supplementary Table 1; Supplementary Fig. 8). To identify other potential caffeoyl derivatives in the extract, the latter was submitted to acid hydrolysis before liquid chromatography–mass spectrometry (LC–MS)/MS analysis, but no trace of caffeoyl residues was found in the mutant (Fig. 3d; Supplementary Table 2). PpCYP98 deletion thus abolished the formation of free and bound caffeic acid.
PpCYP98 is required for the moss cuticle formation
The organ fusion phenotype of the ΔPpCYP98 mutant suggested impaired formation of the cuticle. This was further indicated by greatly increased surface permeability of the mutant gametophore to toluidine blue stain, compared with WT (Fig. 4a, Supplementary Fig. 9), and by transmission electron microscopy, which revealed perturbation of the integrity of the mutant cuticle (Fig. 4b). The composition of the biopolymer, cutin, the main constituent of cuticle, was therefore investigated. A recent study described the presence of a high proportion of phenolic residues in the cutin of P. patens24. Consistent with our observations, the cutin of the ΔPpCYP98 mutant was devoid of caffeate residues (Fig. 4c) and, strikingly, also showed a substantial decrease in native and oxygenated C16 and C18 fatty acids monomers. This decrease in fatty acid content did not reflect fatty acid hydroxylase activity of the PpCYP98 enzyme, which we determined did not catalyse C16 palmitic acid oxygenation (Supplementary Fig. 10). We therefore inferred that caffeic acid, or its derivatives, plays a key role in the cell-wall anchoring or structure of the cutin polymer in P. patens, or contributes to its regulation. Consistent with this hypothesis, addition of caffeic acid to the growth medium of the ΔPpCYP98 mutant partially restored both plant growth and impermeability of the cuticle to toluidine blue (Fig. 4d,e; Supplementary Fig. 11).
Taken together, the free phenolic and polymer analyses indicate that caffeic acid derivatives are the major products of the phenolic metabolism in the moss P. patens. Our data also demonstrate that this moss ‘pre-lignin’ pathway is crucial for the formation of a cuticular biopolymer and that caffeic acid production is a limiting factor in its biosynthesis. Unexpectedly, the substrate for the meta-hydroxylation reaction to form caffeic acid does not appear as free p-coumaric acid or p-coumaroyl-shikimate, but rather as p-coumaroyl-threonate. Threonic acid is a product of ascorbate catabolism25,26 and so we conclude that the formation of caffeic acid in moss is coupled to the hexose-derived ascorbate pathway, rather than the plastidial pentose phosphate-derived shikimate pathway, as is reported for vascular plants (Fig. 1). The importance of ascorbate has been revealed by the conservation of three different biosynthesis pathways in P. patens27. Stresses, including light and desiccation, are likely to regulate the formation of this biopolymer, and possibly the cuticle caffeic acid content, thereby increasing its antioxidant and ultraviolet-screening properties. The composition of the moss cuticle, namely its associating oxygenated phenolics and fatty acids, is more reminiscent of the polyester suberin than of cutin from seed plants5. It clearly confers surface protection and impermeability, and is also likely to contribute to the erect growth and rigidity of the moss gametophore. It may in particular contribute to the rigidity of the gametophore phyllid sheets, which are formed from a single-cell layer24. It has been hypothesized that cutin and suberin might share a common evolutionary origin4. Our data suggest that the lipid–phenolic matrix present in P. patens may constitute an extant representative of the common ancestor of the suberin, cutin and lignin polymers that have been described associated with highly differentiated vegetative tissues in more recently diverged plant lineages. This ancestral structure was presumably critical for the plant transition from water to land, and suggest new strategies for engineering biopolymers to enhance stress tolerance in vascular plants.
Plant material and growth conditions
P. patens (Hedw.) Bruch & Schimp. strain Grandsen6 was cultured in liquid or on solid Knop medium28 supplemented with 50 μmol l−1 H3BO3, 50 μmol l−1 MnSO4, 15 μmol l−1 ZnSO4, 2.5 μmol l−1 KI, 0.5 μmol l−1 Na2MoO4, 0.05 μmol l−1 CuSO4 and 0.05 μmol l−1 CoCl2. Medium was solidified with 12 g l−1 purified agar (OXOID, Thermo Scientific). Plants were kept at 23 °C under 16/8 h day/night cycle, light intensity set to 70 μmol m−2 s−1, and liquid cultures were upheld under constant agitation for proper aeration. Protonema material was grown in liquid cultures and maintained by weekly tissue disruption and subculturing. Gametophores were propagated on agar plates. In some cases, gametophores liquid cultures were established by soft tissue disruption (∼5 s) of individual gametophores. Sporophyte formation was induced in agar plate-grown gametophores by reducing day length and temperature as reported before29.
Generation of transgenic lines
To generate the ΔPpCYP98 knockout mutants, two 750 bp genomic regions were PCR-amplified from P. patens genomic DNA and assembled with the nptII selection cassette into a PCR-linearized pGEM-T vector via GIBSON cloning30 (Supplementary Fig. 3, Supplementary Table 3 for primers). The PpCYP98 disruption construct was excised from the vector backbone by BamHI digestion, using restriction sites introduced during PCR. Twenty-five microgram of linearized construct were used for PEG-mediated transfection of P. patens protoplast31. Transformants were selected on Knop plates supplemented with 25 mg l−1 geneticin (G418).
For PpCYP98:uidA reporter lines, two 800 bp genomic regions framing the PpCYP98 STOP codon were PCR-amplified from P. patens genomic DNA and assembled with the uidA reporter gene into a PCR-linearized pGEM-T vector via GIBSON cloning30 (Supplementary Fig. 2, Supplementary Table 3). A linker DNA sequence was introduced during PCR to limit GUS protein hindrance on PpCYP98 activity (Supplementary Fig. 2). The PpCYP98:uidA construct was excised from the vector backbone by EcoRI digestion, using restriction sites introduced during PCR. Twenty-five micrograms of linearized construct were used for transfection of P. patens protoplast31. The PpCYP98:uidA construct does not harbour a selection cassette and was therefore co-transfected with the pRT101 plasmid32 containing the nptII selection cassette. Transformants were selected on Knop plates supplemented with 25 mg l−1 geneticin (G418).
Molecular characterization of transgenic lines
Following the selection process, a previously established direct-PCR protocol33 was implemented to identify transformants with proper genomic integration of the DNA construct. Briefly, one gametophore or 2–3 protonema filaments were incubated for 15 min at 45 °C in a DNA extraction buffer (9.1 g l−1 Tris-HCl pH 8.8, 2.6 g l−1 (NH4)2SO4, 0.1 ml l−1 Tween 20). PCR reactions were performed with the Phire II polymerase (Thermo Scientific) and 2.5 μl of the DNA extract in 15 μl reaction. Both 5′ and 3′ integrations were verified using appropriate PCR strategy and primers (Supplementary Figs 2 and 3, Supplementary Table 3).
ΔPpCYP98 lines identified by direct-PCR were further validated at the molecular level by conventional PCR with reverse transcription (Supplementary Fig. 3C). To this end, total RNA was isolated from ∼8 mg of lyophilized 3-day-old protonema material using TriReagent (Sigma-Aldrich). Twenty micrograms of RNA were treated with 5U of RQ1 DNaseI (Promega) and subsequently purified with the Nucleospin RNA clean-up XS kit (Macherey-Nagel). One microgram of DNaseI-treated RNA was reverse-transcribed with oligo(dT)23V and the Superscript III enzyme (Thermo Scientific) in 20 μl reaction. PpCYP98 transcripts were amplified from 1 μl of cDNA using the Phire II polymerase (Thermo Scientific) in 20 μl reaction. The constitutively expressed L21 gene (Pp1s107_181V6.1), encoding a 60S ribosomal protein, was used as reference gene.
The number of ΔPpCYP98 lines was narrowed down after transcript analysis; remaining lines were subjected to transgene copy analysis by quantitative PCR as described before34. Genomic DNA was isolated using a protocol adapted from Edwards et al.35. Briefly, nucleic acids were extracted from 5 mg of 3-day-old lyophilized protonema material with 500 μl of lysis buffer (200 mM Tris-HCl pH 8.0, 250 mM NaCl, 25 mM EDTA, 0.5% SDS) and thorough agitation. Nucleic acids were purified by addition of a 500 μl of a phenol:chloroform (1:1) solution (pH 8.0) followed by a precipitation with sodium acetate and isopropanol. DNA pellets were washed with 75% ethanol before solubilization in a 5 mM Tris pH 8.5 solution. Samples were further treated with a RNase A/T1 mix (Thermo Scientific) to remove RNA. DNA was re-purified with a phenol:chloroform step as described above. Typical yields were ∼0.5 μg DNA per mg of dry plant material. Quantitative PCR reactions were run on a LightCycler 480 II device (Roche) in 10 μl comprising 1 ng genomic DNA reaction, 250 nM of each primer and 1X LightCycler 480 SYBR Green I Master mix (Roche). Reactions were performed in triplicate and crossing points were determined using the manufacturer software. Both the 5′- and 3′-homologous regions were targeted using specific primers (Supplementary Fig. 3, Supplementary Table 3). The single-copy gene PpCLF (Pp1s100_146V6.1) was amplified using two primer pairs and served as an internal standard for input amount normalization. Transgene copy number was determined by comparing relative values of the tested genomic segment in transgenic lines with those of the WT. Three ΔPpCYP98 lines with a single transgene copy (Supplementary Fig. 3) were kept for subsequent phenotypic and metabolic analyses.
Plant tissues were vacuum infiltrated with X-Gluc solution (1 mM 5-bromo-4-chloro-3-indolyl-β-glucoronide, 100 mM sodium phosphate and pH 7.0) and incubated at 37 °C for 24 h. The samples were fixed in 5% v/v formaldehyde, 5% v/v acetic acid, 100 mM sodium phosphate and pH 7.0 for 30 min. Chlorophyll was extracted with an ethanol series (30, 50, 70 and 100%).
Recombinant proteins production in yeast and enzyme assays
Procedures were adapted from Liu et al.36. Coding sequence of the P. patens PpCYP98 gene was optimized for yeast expression (sequences available in Supplementary Note 1) and synthesized by GeneCust Europe (Dudelange, Luxembourg) with addition of BamHI and KpnI restriction sites at the 5′ and 3′ termini, respectively. BamHI/KpnI sites were used for subcloning CDS into the yeast expression plasmid pYeDP60.
The Saccharomyces cerevisiae strain WAT11, expressing the ATR1 cytochrome P450 reductase from Arabidopsis thaliana under the control of the galactose-inducible promoter GAL10-CYC1 (ref. 37), was transformed with the pYeDP60:PpCYP98 plasmid and selected on minimum SGI medium (1 g l−1 bactocasamino acids, 7 g l−1 yeast nitrogen base, 20 g l−1 glucose and 40 mg l−1 L-tryptophan). Isolated colonies were chosen for initiating SGI liquid cultures and were grown for 18 h at 28 °C under 160 r.p.m. agitation. Ten millilitres of SGI culture were used to inoculate 200 ml of YPGE medium (10 g l−1 bactopeptone, 10 g l−1 yeast extract, 5 g l−1 glucose and 3% ethanol by volume). Following a 30 h growth period at 28 °C under 160 r.p.m. agitation, production of recombinant proteins was induced by supplementing the growth medium with 10 ml of 200 g l−1 sterile galactose solution. Proteins production phase was performed at 20 °C for 16 h.
Yeast cells were harvested by centrifugation at 7,500g for 10 min at 4 °C, washed with TEK buffer (50 mM Tris-HCl pH 7.5, 1 mM EDTA, 100 mM KCl) and resuspended in 2 ml of TES buffer (50 mM Tris-HCl pH 7.5, 1 mM EDTA, 600 mM sorbitol) supplemented with 5 mM 2-mercaptoethanol and 10 g l−1 bovine serum albumin, fraction V (buffer A). Cell suspensions were transferred to 50 ml conical tubes and homogenized with 0.5 mm glass beads by handshaking five times for 1 min. Beads were washed twice with 30 ml of buffer A. Cell debris and remaining glass beads were removed from the pooled lysates by a 20 min centrifugation step at 7,500g and 4 °C. Supernatants were filtrated on Miracloth (22–25 μm pore size, Calbiochem, MD, USA) and microsomal fractions were purified by differential centrifugation (100,000g, 4 °C, 1 h). Pelleted microsomes were resuspended in TEG buffer (50 mM Tris-HCl pH 7.5, 0.5 mM EDTA, 30% glycerol by volume) with a Potter-Elvehjem homogenizer. Microsomes preparations containing PpCYP98 recombinant proteins were stored at −20 °C until processing.
Enzyme assays were performed in 50 mM potassium phosphate buffer (pH 7.4) containing 100 μM substrate, 10 pmol of PpCYP98 recombinant enzyme and 500 μM NADPH in a final volume of 200 μl. Reactions were initiated by addition of the NADPH, incubated at 28 °C in the dark for 30 min and terminated with 1/10 50% acetic acid and 4/10 acetonitrile. Microsomal membranes were spun down by centrifugation (13,000g, 10 min, 4 °C). Reaction products were analysed from supernatants by Ultra Performance Liquid Chromatography (UPLC)-MS/MS as described below.
Metabolic profiling of Physcomitrella patens
Protonema material was harvested 3 days after tissue disruption. Gametophores grown in liquid medium were harvested 1 month after the last disruption and 1 week after medium change. P. patens tissues were collected by pouring the culture onto a sieve (100 μm pore size) and were thoroughly rinsed with distilled water, quickly blotted on paper towel and finally snap-frozen in liquid nitrogen. Tissues were lyophilized overnight before grinding with 5 mm steel balls and a Tissuelyser II (Qiagen) operated at 30 Hz for 2 min.
Metabolites were extracted with a previously described methanol:chloroform:water protocol38. Briefly, 400 μl of methanol containing 10 μM morin as an internal standard were added to 10 mg of lyophilized ground plant material. After agitation at 1,500 r.p.m. for 1 h, 200 μl of chloroform were added and samples were shaken for five additional minutes. Phase separation was induced by adding 400 μl of ultra-pure water followed by vigorous agitation and centrifugation (15,000g, 4 °C, 15 min). Supernatants were transferred to clean microtubes and constituted the crude extracts. To hydrolyse ester bonds of hydroxycinnamic acid conjugates, 250 μl of crude extract were dried under reduced pressure. Dry residues were resuspended in a 50% methanol solution containing 2 N HCl and 2.5 mg ml−1 ascorbic acid as an antioxidant. Acid hydrolysis was performed at 80 °C for 2 h.
Metabolites separation and detection were carried out on an Acquity UPLC (Waters corp.) coupled to a photodiode array detector (Waters corp.) and a Quattro Premier XE tandem-mass spectrometer (Waters corp.) equipped with an electrospray ionization source. Ten microliters of extract were injected onto a UPLC BEH C18 column (100 × 2.1 mm, 1.7 μm; Waters) outfitted with a pre-column and operated at 35 °C. Metabolites chromatography was performed at a 0.35 ml min−1 flow rate with a mixture of 0.1% formic acid in water (solvent A) and 0.1% formic acid in acetonitrile (solvent B) according to the following programme: initial, 98% A; 11.25 min, 0% A, curve 8; 12.75 min, 0% A, curve 6; 13.50 min, 98% A, curve 6; 15 min, 98% A. Nitrogen was used as the drying and nebulizing in-source gas. The nebulizer gas flow was set to 50 l h−1, and the desolvation gas flow was set to 900 l h−1. The interface temperature was set to 400 °C, and the source temperature to 135 °C. Capillary voltage was set to 3.4 kV. Data acquisition and analysis were performed with the MassLynx v4.1 software (Waters corp.). Metabolites were ionized in positive mode and detected using dedicated multiple reaction monitoring methods (Supplementary Table 4). The QuanLynx module of MassLynx was executed to integrate peaks and to report corresponding areas. Peak areas were normalized to plant dry weight and internal standard level (morin), leading to relative levels. External calibration curves of authentic standards were employed for the absolute quantification of hydroxycinnamic acid after acid hydrolysis.
In vitro assay for palmitic acid conversion
The radiolabelled substrate was dissolved in ethanol that was evaporated before the addition of microsomal fraction into the glass tube. Resolubilization of the substrates was confirmed by measuring the radioactivity of the incubation media. The standard assay (0.1 ml) contained 20 mM sodium phosphate (pH 7.4), 1 mM NADPH, radiolabelled substrate (100 μM) and 35 μl of microsomal fraction. The reaction was initiated by the addition of NADPH and was done in a bathwater 20 min at 27 °C under agitation. Incubation media were directly spotted on thin layer chromatography (TLC) plates. For separation of metabolites from residual substrate, TLC plates were developed with a mixture of diethyl ether/light petroleum (boiling point, 40–60 °C)/formic acid (50:50:1, v/v/v). The plates were scanned with a radioactivity detector (Raytest Rita Star).
Transmission electron microscopy
Samples were fixed overnight in 2% glutaraldehyde and were then treated for 2 h with 2% uranyl acetate 2% (w/v) and then stained with osmium tetroxide 0.1% (v/v) in 150 mM phosphate buffer, pH 7.2. Samples were dehydrated through an ethanol series and infiltrated with EPON812 medium grade resin (Polysciences). Polymerization was allowed for 48 h at 60 °C. Ultrathin sections (70 microns) were cut using an ultracut E microtome (Reichert) and collected on grids coated with formvar (electron microscopy sciences (EMS)). Samples were visualized with a Hitachi H-7500 electron microscope operating at 80 kV.
Tissue permeability was assessed by immersing plants into a 0.05% toluidine blue solution for 2 min. Samples were subsequently thoroughly washed with distilled water until the washing solution was clear.
Cutin monomers analysis
Cutin monomers analysis was performed on the same plant material as used for metabolic analysis (that is, lyophilized gametophores grown in liquid medium). For each sample, ∼200 mg of ground, lyophilized moss tissue was added to a pre-weighed 40 ml glass vial for processing. The tissue was delipidated by extensive washing with a series of solvents, each containing 0.01% butylated hydroxytoluene, as follows.
A total of 40 ml of isopropanol pre-heated to 85 °C was added to each sample and incubated at 85 °C for 15 min, then after cooling to room temperature, the samples were shaken at 250 r.p.m. for 1 h and centrifuged at 1,500g for 5 min to pellet most of the tissue. The supernatant was removed with a glass Pasteur pipette and filtered through a paper filter (Whatman #1) to collect the suspended tissue particles, which were then scraped off the paper and added back to the sample vial. Three more washes (agitation, centrifugation and filtering) were performed, adding 30 ml of room temperature isopropanol each time. The tissue was then washed with the following series of solvents: 2:1 chloroform: methanol (repeated once), 1:2 chloroform: methanol, 1:1 chloroform: methanol, 1:2 chloroform: methanol, pure methanol. The samples were agitated with each of these solvents at 250 r.p.m. for at least 2 h and up to overnight, with centrifugation and filtration (as described above) after each wash. The tissue was then dried under a stream of nitrogen for 20 min and freeze dried overnight. The vial was weighed to determine the dry, delipidated tissue weight.
A total of 8 ml of reaction media (12:3:5 methanol: methyl acetate: 25% sodium methoxide) and 100 μg of each of pentadecalactone and heptadecanoate (internal standards) were added to each sample, and the mixture was then heated at 60 °C overnight to depolymerize the cutin. The samples were then cooled to room temperature and 16 ml dichloromethane, 2 ml glacial acetic acid and 4 ml 0.9% NaCl in 100 mM Tris (pH 8.0) was added to each and vortexed to mix. Two phases were separated by centrifugation for 2 min at 1,500g. The lower phase was transferred to a new vial and 14 ml of 0.9% NaCl in 100 mM Tris (pH 8.0) was added and mixed by vortexing. Two phases were again separated by centrifugation (2 min at 1,500g) and the lower phase was transferred to a new vial, while the upper phase was discarded. Roughly 0.5 g of anhydrous sodium sulfate added to remove any residual water, and the solution then filtered through a paper filter (Whatman #1) into a clean vial.
An aliquot of each cutin sample was dried by heating at 40 °C under a stream of nitrogen, then derivatized with 50 μl each of pyridine and BSTFA (N,O-bis(trimethylsilyl)trifluoroacetamide) for 10 min at 90 °C, dried again by heating under nitrogen, and resuspended in 100 μl chloroform. The samples were analysed by gas chromatography (GC) using an Agilent GC 6850 with a Flame Ionization Detector. Compounds were identified based on a comparison of retention times with standards and also by performing GC–mass spectrometry (MS) using an Agilent GC 6890 coupled to a JEOL GC MATE II mass spectrometer. Cutin levels were normalized to the internal standards and the dry, delipidated tissue weights.
For the chemical complementation of the ΔPpCYP98 plants, caffeic acid (Sigma-Aldrich) was solubilized in absolute ethanol to prepare 100 mM stock solutions. Freshly prepared stock solutions were added to liquid cultures 14 days after the last disruption to a final concentration of 20 μM. After 14 days the medium was exchanged for fresh medium containing caffeic acid. Gametophore development was assessed after 14 and 28 days cultivation in presence of caffeic acid. Control cultures containing 0.05% ethanol were run in parallel.
Chemical synthesis of p-coumaroyl-threonate esters
Detailed procedures are available in Supplementary Note 2.
The data that support the findings of this study are available from the corresponding authors upon request. The transgenic moss lines described in this study are deposited in the International Moss Stock Center (Ahttp://www.moss-stock-center.org/) with the accession numbers IMSC 40805-40814.
How to cite this article: Renault, H. et al. A phenol-enriched cuticle is ancestral to lignin evolution in land plants. Nat. Commun. 8, 14713 doi: 10.1038/ncomms14713 (2017).
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D.W.-R., R.R. and H.R. acknowledge the support of the Freiburg Institute for Advanced Studies (FRIAS) and the University of Strasbourg Institute for Advanced Study (USIAS) to the METABEVO project. D.W.-R. and H.R. also acknowledge support of the Agence Nationale de la Recherche to the LabCom TerpFactory. Support to J.K.C.R. was provided by grants from the US National Science Foundation’s Plant Genome Research Program (IOS-1339287) and by the Agriculture and Food Research Initiative Competitive Grants Program (2011-67013-19399) of the US Department of Agriculture’s National Institute of Food and Agriculture. E.A.F. was supported by a fellowship from NSERC (Natural Sciences and Engineering Research Council of Canada). A.A. acknowledges funding by the Natural Sciences and Engineering Research Council of Canada in the framework of the Collaborative Research and Training Experience Program ‘Working on Walls’ and from the Collège Doctoral Européen. R.R. acknowledges funding by the Excellence Initiative of the German Federal and States governments (EXC 294). N.A.H. is grateful for the support from the People Programme (Marie Curie Actions) of the European Union’s 7th Framework Programme (FP7/2007-2013) under REA Grant Agreement 289217. L.K. and E.P. acknowledge the support of the French Ministry of Education and Research for PhD funding. We thank Dr F. Pinot (IBMP, Strasbourg) for providing the CYP704B1 chromatograms. This paper reflects only the author’s views and the European Union is not liable for any use that may be made of the information contained herein.
Supplementary Figures, Supplementary Tables, Supplementary Notes and Supplementary References
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Plant Cell Reports (2018)