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Copper-containing amine oxidases contribute to terminal polyamine oxidation in peroxisomes and apoplast of Arabidopsis thaliana



Polyamines (PAs) are oxidatively deaminated at their primary or secondary amino-groups by copper-containing amine oxidases (CuAOs) or FAD-dependent amine oxidases (PAOs), respectively. Both enzymes have long been considered to be apoplastic proteins. However, three out of five PAO isoforms in Arabidopsis thaliana are localized in peroxisomes, while the other two PAOs are predicted to be cytosolic. Interestingly, most of these PAOs do not contribute to terminal PA oxidation, but instead are involved in the back-conversion pathway, producing spermidine from spermine and putrescine from spermidine, which in turn is inhibited by putrescine. This opens the question as to whether PAs are catabolized in the apoplast of Arabidopsis and if the terminal oxidation occurs in the peroxisomes. The main objective of this study was to know if these catabolic processes are mediated by CuAOs.


A. thaliana contains ten genes annotated as CuAOs, but only one (ATAO1) has been characterized at the protein level. Reported herein is the characterization of three genes encoding putative Arabidopsis CuAOs (AtCuAO1, AtCuAO2 and AtCuAO3). These genes encode functional CuAOs that use putrescine and spermidine as substrates. AtCuAO1, like ATAO1, is an extracellular protein, while AtCuAO2 and AtCuAO3 are localized in peroxisomes. The three genes present a different expression profile in response to exogenous treatments, such as application of abcisic acid, methyl jasmonate, salycilic acid, flagellin 22 and wounding.


PA catabolism in the Arabidopsis apoplast is mediated predominantly by CuAOs, while in peroxisomes the co-localization of CuAO-dependent terminal catabolism with PAO-back-conversion machineries might contribute to modulating putrescine-mediated inhibition of the back-conversion, suggesting the occurrence of a tight coordination between both catabolic pathways. The expression profile of AtCuAO1-3 in response to different exogenous treatments, together with the different localization of the corresponding proteins, provides evidence for the functional diversification of Arabidopsis CuAO proteins.


The polyamines (PAs) putrescine (Put), spermidine (Spd), and spermine (Spm) are low-molecular-weight organic cations found in a wide variety of organisms. In plants, polyamines are involved in different physiological processes, such as growth, development, and response to abiotic and biotic stresses [14].

PAs are oxidatively deaminated by amine oxidases (AOs), including those that are FAD-dependent (PAO, EC and copper-containing (CuAO, EC [5]. PAOs catalyse the oxidative deamination of Spm, Spd and/or their acetylated derivatives at the secondary amino group [6]. The chemical identity of PAO reaction products depends on the enzyme source and reflects the mode of substrate oxidation. Thus, in monocotyledonous plants, PAOs catalyse the terminal catabolism of PAs oxidizing the carbon at the endo-side of the N4-nitrogen of Spd and Spm to produce 4-aminobutanal and N-(3-aminopropyl)-4-aminobutanal, respectively, in addition to 1,3-diaminopropane (DAP) and H2O2[6, 7]. In contrast, in the dicotyledonous model plant Arabidopsis thaliana, PAOs, namely AtPAO1, AtPAO2, AtPAO3 and AtPAO4, oxidize the carbon at the exo-side of the N4-nitrogen of Spd and Spm, giving rise to a PA back-conversion pathway, with the production of Spd from Spm and Put from Spd, in addition to 3-aminopropionaldehyde and H2O2[812].

CuAOs catalyse the oxidation of PAs at the primary amino group, giving the corresponding aminoaldehydes, with concomitant production of H2O2 and NH3, but in contrast to PAOs, they are unable to produce the oxidative splitting of PAs by reaction with secondary and tertiary amino groups [13, 14]. CuAOs are homodimeric proteins, consisting of 70–90 kD subunits, each containing a copper ion and a 2,4,5-trihydroxyphenylalanine quinone cofactor (TPQ) generated by a post-translational autocatalytic modification of a tyrosine residue in the active site [15]. Although the overall primary sequence identity of CuAO from different sources is usually not high (<25%) [14], thirty-three amino acid residues near the catalytic site are fully conserved in most of them [16, 17].

Plant AOs contribute to important physiological processes, including plant growth and development, response to abiotic stresses such as drought, salinity, and heat, and defence responses against pathogens [6, 7]. These effects are mediated not only through the regulation of cellular PA levels, but mainly by the AO reaction products: aminoaldehydes, GABA (γ-aminobutiric acid) and, markedly, H2O2[1, 2, 6, 7, 18].

CuAOs and PAOs, abundant in the apoplast of Fabaceae and Gramineae, respectively, have long been considered characteristic of these two plant families, leaving PA catabolism uncovered in other plant families and underestimating their potential contribution in other cellular compartments. More recently, a number of CuAOs and PAOs have been detected in several taxa and the occurrence of AOs in intracellular compartments has been demonstrated [6, 7]. Indeed, a peroxisomal localization has been reported for three of the five PAO isoforms present in A. thaliana (AtPAO2, AtPAO3 and AtPAO4), while the other two (AtPAO1 and AtPAO5) are predicted to be cytosolic proteins [12]. Moreover, as mentioned above, the AtPAOs oxidize PAs through the back-conversion pathway [12]. Questions then arise as to whether some AOs, localized in the same subcellular compartment as the Arabidopsis PAOs, are able to catalyse the terminal oxidation of PAs and how PAs are oxidized in the apoplast of this model plant. CuAOs occur at high levels in dicots and are the most abundant soluble protein detected in the extracellular fluids of several Fabaceae (pea, chickpea, lentil and soybean) [19]. The genome of A. thaliana contains ten genes annotated as copper-binding amine oxidases, but only one (ATAO1) has been characterized at the protein level, and it has been predicted that ATAO1 is an extracellular protein [17].

In this work, we have characterized three of the other nine genes encoding putative CuAOs in Arabidopsis (At1g62810, At1g31710 and At2g42490). Our results indicate that these genes encode functional CuAOs with differential cellular localizations in the apoplast and peroxisomes. The expression profile of these genes in different tissues and in response to several exogenous stimuli point to a potential specification in their biological roles. Finally, considering our results and previous reports, we propose a model by which PA catabolism can be accomplished in Arabidopsis.


AtCuAO1, AtCuAO2 and AtCuAO3sequence comparison

In various plant species CuAO genes consist of a multigene family [16, 17]. A search of the Arabidopsis genome database revealed the presence of ten genes encoding putative CuAOs (Table 1). We selected the three more highly expressed genes in the GENEVESTIGATOR database ( [20] for further studies: At1g62810 (AtCuAO1[21]), At1g31710 (referred to as AtCuAO2) and At2g42490 (referred to as AtCuAO3). The deduced amino acid sequences of these three putative Arabidopsis CuAOs were aligned with other known plant CuAOs (Figure 1). AtCuAO1 and AtCuAO2 showed a high level of sequence conservation relative to previously characterized plant CuAOs, with a lower level observed in AtCuAO3. In particular, the amino acid sequence of AtCuAO1 exhibited 60% similarity to ATAO1 and 64% to the CuAO of Pisum sativum (PsCuAO) [GenBank: L39931]. The amino acid sequence similarity between AtCuAO2 and ATAO1 was 65%, and 71% between AtCuAO2 and PsCuAO. However, the sequence similarity of AtCuAO3 with ATAO1 and PsCuAO was lower, 45% and 44%, respectively. The amino acid sequence similarity between AtCuAO3 and the other two AtCuAOs was also low, 44% with AtCuAO2 and 43% with AtCuAO1, while AtCuAO2, exhibited 63% similarity with AtCuAO1. Amino acid residues shown to be important for the catalytic activity of plant CuAOs are apparently conserved in the three AtCuAOs studied in this work (Figure 1). ATAO1 contains 32 of the 33 amino acid residues that have been reported to be fully conserved in CuAOs from different sources [16, 17], while AtCuAO1, AtCuAO2 and AtCuAO3 contain 32, 31 and 30 of these amino acids, respectively (Figure 1), including the active site tyrosine (Figure 1, Tyr441, Tyr412, Tyr495), which undergoes modification to form the TPQ cofactor [22, 23], four histidines, three of which correspond to copper ligands [24, 25] (Figure 1; His499, His501 and His662 for AtCuAO1; His472, His474 and His632 for AtCuAO2; His546, His548 and His712 for AtCuAO3) and the aspartic acid active site base [26] (Figure 1, Asp354, Asp325 and Asp412).

Table 1 Genes annotated as copper-containing amine oxidases in The Arabidopsis Information Resource (TAIR) database
Figure 1
figure 1

Amino acid sequence alignment of AtCuAO1, AtCuAO2 and AtCuAO3 with other plant CuAOs. Organism symbols (GenBank accession numbers): AtCuAO1 (NM_104959), AtCuAO2 (NM_102906), AtCuAO3 (AY120717) and ATAO1 (NM_117580), Arabidopsis thaliana CuAOs; PsCuAO (L39931), Pissum sativum CuAO. Identical residues are marked with asterisks. Conserved and semi-conserved substitutions are denoted by ‘:’ and ‘.’, respectively. The 33 residues totally conserved in most of the CuAOs are indicated by grey boxes. The residues not conserved in the A. thaliana CuAOs are inversely highlighted. The copper binding histidine residues and the tyrosine modified to TPQ are marked with $ and @, respectivelly. The aspartic acid active site base is indicated by #. The peroxisomal targeting signal of AtCuAO3 is underlined. The analysis was accomplished using the ClustalW sequence alignment.

Expression of AtCuAO1, AtCuAO2 and AtCuAO3 in N. benthamianaand characterization of the recombinant-TAP fusion protein

To ensure that AtCuAO1, AtCuAO2 and AtCuAO3 encode functional CuAO enzymes, they were transiently expressed in N. benthamiana as fusion proteins using the plant expression vector pC-TAPa [27]. The TAP (tandem affinity purification) tag, lying downstream of the AtCuAO1, AtCuAO2 and AtCuAO3 ORFs, facilitates antibody detection and protein purification.

AtCuAO1, AtCuAO2 and AtCuAO3 encode 712-, 681- and 776-amino acid proteins, respectively, with calculated molecular masses of 80.1, 76.7 and 86.7 kD, while the TAP has a calculated molecular mass of 34.3 kD.

Five days after agro-infiltration, tissues were harvested, and the soluble protein extracts were analyzed by western blot using anti-myc epitope antibodies. A single band of the expected size (114 kD, 111 kD and 121 kD) was observed for each of the three fusion proteins (AtCuAO1-TAP, AtCuAO2-TAP, AtCuAO3-TAP) (Figure 2B), which were purified by affinity chromatography using IgG-Sepharose beads and digestion with 3C protease for IgG cleavage. In the partially purified extracts the antibodies detected bands of about 101, 98 and 108 kD, which correspond to the size expected for the fusion proteins without the 2xIgG binding domain of protein A: AtCuAO1-MYC9-His6, AtCuAO2-MYC9-His6 and AtCuAO3-MYC9-His6, respectively (Figure 2B). Enzyme activity of each fusion protein was evaluated by the H2O2 production. For this, the proteins were incubated with the H2O2-sensitive Amplex red reagent, peroxidase and either Put, Spd or Spm. When any of the three proteins were incubated with Put significant oxidase activity was detected (Figure 2C), which was reduced by pre-treatment with aminoguanidine (AG), an irreversible competitive inhibitor of amine oxidases that interacts with the TPQ cofactor (Figure 2C). The oxidase activity was also reduced by pre-treatment with the copper complexing agent 8-hydroxyquinoline (8HQL), a non-competitive inhibitor of CuAOs (Figure 2C). Spd was also a good substrate for the three proteins, and the enzyme activity was again inhibited by AG and 8HQL (Figure 2C). However, none of the three fusion proteins recognised Spm as a substrate. These results suggest that AtCuAO1, AtCuAO2 and AtCuAO3 encode functional CuAOs able to oxidize Put and Spd, but not Spm, with the subsequent release of H2O2.

Figure 2
figure 2

Expression and activity of recombinant AtCuAO1, AtCuAO2 and AtCuAO3 proteins. (A) Construct used to produce recombinant AtCuAOs in N. benthamiana: The PCR-amplified CuAO ORFs without the stop codon flanked by Gateway recombination cassette sequences were cloned in-frame with the TAP tag composed of: two copies of the protein A IgG binding domain, the 3C protease cleavage site, a six histidine stretch, and nine repeats of the myc epitope. The expression of TAP-tagged AtCuAOs is under the control of the duplicated 35S cauliflower mosaic virus promoter (2x35S), a tobacco mosaic virus translational enhancer (TMV-Ω), and a NOS terminator (NOSt). RB, T-DNA right border sequence; LB, T-DNA left border sequence. (B) Western blot analyses of recombinant AtCuAO proteins produced in N. benthamiana plants. Proteins present in total extract (TE) and in the eluate, obtained from IgG beads using 3C protease (+3C), were separated on an 8% SDS-PAGE gel and immunoblotted using the α-myc antibody. The highest MW band corresponds to the fusion protein containing the whole TAP-tag, while in the lower MW band the IgG binding domain has been cleaved. Molecular weight markers (kD) are shown on the right. (C) Amine oxidase activity of recombinant fusion proteins AtCuAO1-MYC9-His6 (AtCuAO1), AtCuAO2-MYC9-His6 (AtCuAO2) and AtCuAO3-MYC9-His6 (AtCuAO3) (1 μg) was determined as fluorescence corresponding to the amount of H2O2 released by oxidation of Put or Spd (1 mM), alone or pre-treated with the CuAO inhibitors aminoguanidine (AG, 0.5 mM) or 8-hydroxyquinoline (8HQL, 30 μM), using Amplex Red. Data are the means ± SE of three replicates. Bars represent standard errors.

Subcellular localization of AtCuAO1, AtCuAO2 and AtCuAO3

AtCuAO3 contains at its C-terminus (amino acids 774–776, Figure 1) the canonical SKL tripeptide, involved in the protein targeting to the peroxisome matrix. In fact, the peroxisomal association of this protein has been demonstrated previously by proteome data and a subcellular targeting study of YFP fusion protein [28, 29]. The subcellular localization of this protein was confirmed experimentally by transiently expressing an N-terminal fusion of AtCuAO3 to the YFP in agroinfiltrated N. benthamiana leaf cells (Figure 3I-L). In silico protein localization prediction using PSORT, the only program specifically able to predict peroxisomal targeting, failed to identify any of the other nine Arabidopsis CuAOs as putative peroxisomal proteins. For AtCuAO2, the SUBA database (The Subcellular Location of Proteins in Arabidopsis Database) [30] returned a wide range of possible localizations, including extracellular, plastids, endoplasmic reticulum and cytosol, while for AtCuAO1 the possible localizations were: apoplast, vacuole, endoplasmic reticulum or mitochondria. In order to determine experimentally the subcellular localization of these two AtCuAO isoforms, YFP was fused in-frame to the C-terminus of AtCuAO1 and AtCuAO2. AtCuAO1-YFP and AtCuAO2-YFP were then transiently expressed by Agrobacterium-mediated infiltration of N. benthamiana leaves (Figure 3A-H). Confocal laser microscopy analysis of the transfected cells revealed that, as observed for YFP-AtCuAO3 (Figure 3I-L), the cells expressing AtCuAO2-YFP showed a punctuate fluorescence pattern (Figure 3E). The peroxisomes in the cells were labeled with blue fluorescence (Figure 3F ) due to the co-expression of the peroxisomal marker CFP-SKL [31]. As shown in Figure 3 (C, D, G and H), all punctuated yellow fluorescent signals in the cells coincided with the blue fluorescence of CFP-SKL, confirming that AtCuAO3 is a peroxisomal protein and strongly suggesting that AtCuAO2 is also localized in peroxisomes. Cells expressing AtCuAO1-YFP displayed a pattern of secretion, with fluorescence mainly located in the periphery of the cells (Figure 3A) as occurred in cells expressing Spg-DsRed (Figure 3B), used as a control of protein secretion [32]. Moreover, the yellow fluorescence of AtCuAO1-YFP colocalized with the red fluorescence of the secreted DsRed (Figure 3C and D), suggesting that AtCuAO1 is an extracellular protein.

Figure 3
figure 3

Subcellular localization of YFP-tagged AtCuAO1, AtCuAO2 and AtCuAO3 proteins. Confocal microscopic images showing the fluorescence localization in agroinfiltrated N. benthamiana epidermal leaves transiently co-expressing AtCuAO1-YFP (A) with the extracellular protein marker Spg-DsRed (B) or AtCuAO2-YFP (E) or YFP-AtCuAO3 (I) with the peroxisome protein marker CFP-SKL (F, J). Co-localization evaluation of YFP-tagged AtCuAO proteins with the extracellular (C and D) and peroxisome (G, H, K and L) protein markers. Differential interference contrast (DIC) images showing the morphology of transformed cells and merging between the protein of interest, fused to YFP, and the marker (D, H and L). The data presented are from a single representative experiment that was repeated at least three with similar results. Data were obtained using a 40x water immersion objective.

Spatial and temporal expression of three Arabidopsis CuAOs

To evaluate whether the different CuAO transcripts were spatially regulated, expression of AtCuAO1-3 was examined by real-time RT-PCR using total RNA isolated from different organs of mature Arabidopsis plants (rosette leaves, stems, flowers). The expression of these genes was also determined in 4-, 12-, 21- and 28-day-old whole seedlings to know if there is some kind of regulation during plant development (Figure 4).

Figure 4
figure 4

Expression analyses of AtCuAO genes. The expression of AtCuAO1-3 was determined in 4- to 28-day-old A. thaliana seedlings (white bars) and in different organs of 6-week-old plants (black bars). L, rosette leaves; S, stems; F, flowers. Transcript levels were determined by quantitative RT-PCR using gene-specific primers designed for AtCuAO1, AtCuAO2 and AtCuAO3 and are shown relative to Actin2 in each sample. Values are the mean ± SE from three replicates. Bars represent standard errors.

AtCuAO1, AtCuAO2 and AtCuAO3 transcripts were detected in all organs analysed. AtCuAO1 transcripts were abundant in rosette leaves, but with the highest levels found in stems and flowers. The expression of this gene increased about 3-fold in 28-day-old seedlings when compared with those 4 days old (Figure 4). A similar expression pattern was observed for AtCuAO3, with transcript levels increasing during plant development and, reaching a peak in flowers of adult plants, followed by leaves and stems (Figure 4). In contrast, AtCuAO2 transcript levels, which were abundant in stems but low in other organs, were not observed to increase during the developmental stages (Figure 4).

Transcriptional profile of AtCuAO1-3in response to external stimuli

CuAOs have been reported to be involved in plant response to abiotic and biotic stresses (reviewed by [6] and [7]). Thus, we decided to investigate the expression pattern of AtCuAO1, AtCuAO2 and AtCuAO3 in response to external stimuli by subjecting Arabidopsis seedlings to different treatments, including wounding, flagellin 22 (a pathogen elicitor that activates the plant basal defence), abcisic acid (ABA), salycilic acid (SA), methyl-jasmonate (MeJA), and the ethylene precursor 1-aminocyclopropane-1-carboxylic acid (ACC) (Figure 5).

Figure 5
figure 5

Expression of AtCuAO genes in Arabidopsis seedlings in response to exogenous treatments. Transcript levels of AtCuAO1, AtCuAO2 and AtCuAO3 genes were determined by real-time RT-PCR in Arabidopsis seedlings exposed or not to wounding or treatment with flagellin 22, SA, MeJA, ACC or ABA after 0, 3, 8 and 24 h of treatment. Values are expressed normalized to Actin 2 and relative to non-treated plants at each time point, which is assumed to be one. Values are the mean ± SE of three replicates. Bars represent standard errors.

The highest expression of AtCuAO1 was observed after 24 h in SA-treated plants (about 7.5-fold higher than basal level). At this time point the AtCuAO1 transcripts were also up-regulated in response to MeJA, flagellin and ABA, although at lower degree (about 3.5-fold). It is noteworthy that induction of this gene by ABA was already observed at 3 h post-treatment (Figure 5). AtCuAO1 expression was not significantly affected by wounding and ACC treatment (Figure 5). AtCuAO3 transcript accumulation was also induced by ABA, SA, flagellin and MeJA, at 8 h post-treatment (Figure 5). At 24 h the transcript levels of this gene increased in MeJA-treated plants and decreased in those exposed to ABA or SA, while they were similar to those detected after 8 h of flagellin treatment. AtCuAO3 transcript abundance was slightly lower 8 h after wounding but returned to basal levels after 24 h, and was not significantly affected by ACC treatment (Figure 5). In contrast, while AtCuAO2 expression was clearly induced (about 12-fold) in wounded and MeJA-treated plants at 8 h, it was not affected by any of the other applied treatments (Figure 5).


In Arabidopsis most studies on PA oxidation have been focused on the PAO-mediated back-conversion pathway, but little is known about the terminal oxidative deamination that leads to depletion of PA levels, which in most organisms is considered to be accomplished by CuAOs [3335]. In this study, we have characterized three of the ten genes encoding putative CuAOs in Arabidopsis (At1g62810, At1g31710 and At2g42490), referred to as AtCuAO1, AtCuAO2 and AtCuAO3. The recombinant fusion proteins AtCuAO1-MYC9-His6, AtCuAO2-MYC9-His6 and AtCuAO3-MYC9-His6 are able to oxidize Put and Spd, but not Spm, with the corresponding delivery of H2O2, and this oxidation is inhibited by the CuAO inhibitors AG and 8HQL (Figure 2). These results demonstrated that the three studied genes encode functional CuAOs, which oxidize Put and Spd. Put has been described as the best substrate for most of the characterized CuAOs, but these enzymes are also able to oxidize Spd and Spm in plants and animals [13, 14, 35] All plant CuAOs thus far characterized and the intracellular animal CuAOs have a lower catalytic efficiency for Spd and Spm than Put, while animal serum CuAOs preferentially oxidize Spd and Spm [35]. Thus, Spm oxidation by some of the Arabidopsis CuAOs not yet characterized cannot be discarded.

AtCuAO2 and AtCuAO3 are localized in peroxisomes (Figure 3E-L), thus representing the first CuAOs involved in a peroxisomal catabolic pathway of PAs, since any of the animal or plant CuAOs characterized so far are localized in these organelles [34, 35]. AtCuAO3 contains a peroxisome targeting signal (PTS) at its C-terminus (SKL, Figure 1) and has already been reported as a peroxisomal protein [28, 29]. Although in silico protein localization prediction failed to identify AtCuAO2 as a putative peroxisomal protein, the localization pattern observed using in vivo targeting analysis of CuAO2-YFP fusion protein strongly suggests that it is also a peroxisomal protein (Figure 3E-H). This lack of correlation between in silico predictions and in vivo targeting analysis has been observed in other peroxisomal proteins and could be attributed to an insufficient knowledge of PTS variant sequences or to the action of “piggy-backing” import mechanisms that do not involve PTS sequences [29].

Although AtCuAO3 has been identified as a peroxisomal protein, no experimental data about its function have been reported so far. The results of this work, which show that this protein, as well as AtCuAO2, oxidizes Put and Spd (Figure 2C), acquire special significance considering that none of the three AtPAOs localized in peroxisomes are able to oxidize PAs through a terminal catabolic pathway [12]. Consequently, the terminal oxidation of PAs in these organelles would be mediated by AtCuAO2 and AtCuAO3, thus avoiding the accumulation of Put, which has been described as having an inhibitory effect on the back-conversion pathway [9]. The oxidation of Put produces 4-aminobutanal, which can be further metabolized to GABA by the action of an aldehyde dehydrogenase (ADH) [36]. In Arabidopsis this process could take place in the peroxisomes mediated by a betaine aldehyde dehydrogenase (BADH) found in this organelle (ALDH10A9) [37], which possesses both betaine- and amino-aldehyde dehydrogenase activities, and can oxidize 4-aminobutanal [37] (Figure 6). These results suggest the occurrence of a tight coordination between back-conversion and terminal catabolism pathways to maintain PA homeostasis. The cooperation of the two PA catabolic enzymes is known to occur in the tobacco apoplast, where PAOs catalyse the terminal oxidation of Spd and Spm [38, 39] but, to our knowledge, this is the first time that this cooperation has been reported in peroxisomes, where PAOs are involved in the PA inter-conversion reactions.

Figure 6
figure 6

Schematic representation of polyamine catabolic pathways in Arabidopsis. (A) In the cell wall, Put and Spd can be oxidatively deaminated by CuAOs (ATAO1 and AtCuAO1) to produce the corresponding aminoaldehydes, H2O2 and NH3. (B) In peroxisomes, Spm and Spd are substrates for PAOs (PAO2-4) that catalyse the sequential back-conversion of Spm to Spd and Spd to Put, which is subjected to feedback inhibition by its end product, Put. CuAOs (AtCuAO2 and AtCuAO3) can catalyse the terminal oxidation of Put and Spd. The oxidation product of Put, 4-aminobutanal, can be a substrate for peroxisomal BADH (ALDH10A9), which catalyses its conversion to GABA. (C) In the cytosol, AtPAO1, and probably AtPAO5, oxidize Spm and Spd by the back-conversion pathway. Some AtCuAOs, annotated as cytosolic in TAIR, could mediate terminal PA catabolism in this cellular compartment.

AtCuAO1 is annotated as an extracellular protein in The Arabidopsis Information Resource (TAIR). This localization was experimentally confirmed using in vivo targeting analysis of the YFP-CuAO1 fusion protein (Figure 3A-D). ATAO1, the only AtCuAO isoform characterized hitherto, has also been predicted to be an extracellular protein [17]. Since none of the characterized AtPAOs are localized in the apoplast [19], our data suggest that in the Arabidopsis cell wall the oxidative catabolism of PAs is mediated mainly (or exclusively) by CuAOs.

AtCuAO3, like AtPAO3[9], was up-regulated in response to ABA, MeJA, SA and flagellin (Figure 5). ABA-induction has also been observed in the other two genes encoding peroxisomal AtPAOs (AtPAO2 and AtPAO4) [9], as well as in ALDH10A9[37]. These data support the idea of cooperation between the two PA catabolic pathways in Arabidopsis peroxisomes and suggest that PA catabolism in this organelle can be involved in the plant response to stress. In contrast to AtCuAO3, AtCuAO2 was strongly induced by wounding and MeJA, but not by other stimuli (Figure 5). Therefore, both enzymes might play different roles in defence responses, AtCuAO2 being more specifically involved in the response to mechanical damage. The involvement of CuAO in wound-healing has been previously described in several plant species, such as chickpea, where CuAO expression was strongly induced by wounding and jasmonic acid [40], or pea, where injury induced an increase in CuAO, ADH and peroxidase activity levels, as well as in Put, Spd and GABA content [41]. In tobacco, both PAO and CuAO have been reported to participate in the wound-healing process [7, 39, 42]. On the other hand, the transcript level of AtCuAO3 increased in 28-day-old seedlings compared to those 4 days old, but this was not observed in AtCuAO2 (Figure 4), suggesting that the former gene could have a more relevant role in development. The expression profile of AtCuAO1 (Figure 4) in growing seedlings was similar to that observed for AtCuAO3, suggesting that this gene could also be involved in plant development. It has been reported that the H2O2 produced by plant PA catabolism is necessary for several plant developmental processes, such as cell expansion, polar growth, gravitropism, flower development, stomata aperture and stress responses [35].

AtCuAO1, like AtCuAO3, was up-regulated by ABA, MeJA, flagellin and, to a higher degree, by SA (Figure 5), suggesting that AtCuAO1, like the peroxisomal CuAOs, could also be involved in the plant response to stress, but more studies are required to understand the role of each protein in these processes. Induction of AtCuAO1 by ABA has been previously observed by Wimalasekera et al. [21], who showed that cuao1 mutants present an ABA-hyposensitive phenotype and impaired H2O2 and NO production. Moreover, these mutants were less sensitive to the inhibition of root growth induced by osmotic stress [21], supporting the idea that AtCuAO1 is involved in plant response to abiotic stress. The contribution of apoplastic PA catabolism to stress defense responses has been described in other plant species using PAO-specific inhibitors and transgenic plants [34, 35]. Thus, using transgenic tobacco plants overexpressing (S-PAO) or downregulating apoplastic PAO (A-PAO), Moschou et al. [43] demonstrated that salinity induces the exodus of Spd into the apoplast, where it is catabolized by PAO producing H2O2 that induces either tolerance responses or programmed cell death, depending on the levels of intracellular PAs. Moreover, S-PAO plants were more tolerant to specific pathogens that depend of the apoplast for their growth, like the bacteria Pseudomonas syringae and the oomycete Phytophora parasitica var. nicotianae. Furthermore, the high PA oxidation in the apoplast of these plants preinduces responses such as the expression of SAR-linked genes and increased cell wall-based defense, showing that PAO is a nodal point in a specific apoplast-localized plant-pathogen interaction, at time that induces defense responses to prevent pathogen colonization [44]. Since none of the AtPAOs are localized in the apoplast, it could be hypothesized that the protective roles attributed to apoplastic PAO in tobacco could be mediated by CuAOs in Arabidopsis. Further studies using knock-out mutants or CuAO overexpressor lines might help to verify this hypothesis. It is worth noting that AtCuAO1 was strongly induced by SA, while AtCuAO2 expression increased markedly in response to MeJA (Figure 5). SA and jasmonic acid induce resistance to biotrophic and necrotrophic pathogens, respectively [45]. Thus, the different response of AtCuAO1 and AtCuAO2 to these compounds, together with the different localization of the corresponding proteins (Figure 3), suggest a divergent evolution of CuAO family members leading to specificities in the response to biotrophic and necrotrophic pathogens. Indeed, in tobacco leaf apoplast, PA oxidation has been reported to have a beneficial effect in defence against biotrophic pathogens, while the opposite was observed for necrotrophic pathogens [35, 46].

Overall, our results support that PA catabolism in Arabidopsis occurs in different cellular compartments mediated by different AOs (Figure 6). In the apoplast, Put and Spd are oxidized through a terminal process mediated by CuAOs (ATAO1, AtCuAO1), while in peroxisomes this pathway (catalysed by AtCuAO2 and AtCuAO3) is co-localized with the PAO-mediated back-conversion. In the cytosol, AtPAO1, and probably AtPAO5, catalyse the PA inter-conversion reactions [12]. Some of the putative AtCuAOs are annotated as cytosolic by TAIR, but no experimental data about their function and cell localization are available. Thus, the possibility of co-localization of both PA catabolic pathways in the cytosol cannot be discarded.


Three Arabidopsis CuAOs involved in the terminal catabolism of Put and Spd, two major PAs present in plants, have been characterized. Our results indicate the occurrence of a differential localization of these CuAOs in the apoplast and peroxisomes, together with a possible functional specification of CuAOs against different types of stress. Importantly, our results support that back-conversion and terminal PA catabolism are co-localized in peroxisomes of Arabidopsis, thus suggesting that PA homeostasis is maintained by a tight coordination between both catabolic enzyme machineries (Figure 6). We propose a plausible and integrative model by which PA catabolism can be accomplished in Arabidopsis (Figure 6).


Sequence analysis and plasmid acquisition

Genomic database searches were performed using The Arabidopsis Information Resource (TAIR) database. Multiple sequence alignment of the amino acid sequences was done using the program ClustalW [47]. The plant expression vectors pYL436 [pC-TAPa, Gene Bank: AY737283] [27], pEarleyGate101 and pEarleyGate104 [48], as well as the plasmid containing the coding region of CuAO1 fused to a TAP tag (DKLAT1G62810) were obtained from the Arabidopsis Biological Resource Centre (ABRC) ( (stocks CD3-679, CD3-683, CD3-686 and DKLAT1G62810, respectively). The peroxisomal marker, CFP-SKL [31] was also purchased by the ABRC (Stock CD3-977), while the extracellular marker Spg-DsRed [32] was kindly provided by Dr. MD Ludevid (Center for Research in Agricultural Genomics, Barcelona, Spain).

Plant materials, growth conditions and treatments

Arabidopsis thaliana accession Columbia (Col-0) plants grown in soil or sterile seedlings were used in this work. For growth on soil, seeds were sown in pots containing a mixture of soil, perlite and vermiculite (1:1:1, v/v/v). To obtain sterile seedlings, surface sterilized seeds were sown in plates containing half-strength MS medium [49] supplemented with 1% (w/v) sucrose and solidified with 0.8% (w/v) plant agar (Duchefa Biochemie, Belgium). All seedlings and plants were stratified for 3 d at 4°C in the dark before being transferred to a growth chamber under 16 h /8 h light/dark cycles, at 100 mE m–2 s–1 of light intensity and a temperature of 22°C.

For treatment of seedlings with different compounds, 7-day-old seedlings, grown in MS-plates in a vertical position, were transferred to 6 well tissue culture clusters (10 seedlings/well) containing 8 ml of MS medium without agar and grown in the same conditions. After 10 days, the medium in the wells was removed and 8 ml of fresh medium, containing the different compounds to be tested: 500 μM SA, 100 μM MeJA, 20 μM ACC, 100 μM ABA or 1 μM flagellin 22, was added. Wounding was performed by thoroughly crushing the plantlets with forceps as described by [50].

RNA isolation and quantitative RT–PCR analysis

RNA isolation and real-time PCR analyses were performed essentially as described by [51]. Total RNA from plant tissue was isolated using the TRIzol reagent (Invitrogen Life Technologies, Carlsbad, CA, USA) and subjected to DNase I RNase-free treatment (Invitrogen Life Technologies) to avoid amplification from genomic DNA. After checking the RNA in agarose gel, the samples were subjected to RT-PCR reactions using the Super-Script III first-strand synthesis system (Invitrogen Life Technologies). Real-time PCR assays were performed in quadruplicate with SYBR Green I Master (Roche Applied Science, Mannheim, Germany) using a Light Cycler 480 detection system (Roche). Specific primer sets were designed for AtCuAO1, 5’- AGCTGGCGACATTCTGAGAT-3’ (forward) and 5’-GTCCAGCATCATCCTCCCTA-3’ (reverse); AtCuAO2, 5’-GTCAAGATGGAACTCCCGC-3’ (forward) and 5’-TCGCCACATGATATCTCCAG-3’ (reverse), and AtCuAO3, 5’-GTAAGTTTGTGCCACTCCCCC-3’ (forward), 5’-GCCACTCGACAAAGTAACCCC-3’ (reverse). The amount of target mRNA was normalized by using Actin2 as a housekeeping gene [52]. Experiments were repeated at least three times.

Plasmid construction

The coding regions of AtCuAO2 and AtCuAO3 were amplified by RT-PCR from total RNA of A. thaliana leaves using the following gene-specific oligonucleotides: AtCuAO2-FWD (5’-CACCATGGCTCCACTTCAC-3’) and AtCuAO2-REV (5’-AAGATCGTTTTTAGGAGTGCAC-3’), AtCuAO3-FWD (5’-CACCATGGCCTCAGCTTCGAA-3’) and AtCuAO3-REV (5’-GCGAAGCTTTGAAAGTAAACCAGTCT-3’). The underlined regions in the forward primers facilitate the directional incorporation of the insert into the vector, and the reverse primers were designed to eliminate the stop codon. To maintain the stop codon of AtCuAO3 cDNA, the AtCuAO3-REV-stop primer (5’-AAGCTTTGAAAGTAAACCAGTCTGA-3’) was used in combination with AtCuAO3-FWD. The PCR products were purified using the QIAquick gel extraction kit (Qiagen, CA, USA) and cloned into the pENTR/D-TOPO vector using Gateway technology according to the protocol provided by the manufacturer (Invitrogen Life Technologies). After being checked by sequencing, the inserts were transferred into the plant expression vectors pC-TAPa, pEarlyGate101 or pEarlyGate104. Cloning of the inserts into the pC-TAPa vector yielded the plasmids AtCuAO2-pC-TAP and AtCuAO3-pC-TAP. AtCuAO1-pC-TAP was obtained from the ABRC stock center (DKLAT1G62810). These plasmids, used for production and purification of the recombinant fusion proteins, contain the AtCuAO1-3 coding sequences, fused at their C-terminus to a TAP tag, composed of two copies of the immunoglobulin-binding domain of protein A from Staphylococcus aureus, a human rhinovirus 3C protease cleavage site, a six histidine repeat and nine myc epitopes [27]. This is flanked by two copies of the cauliflower mosaic virus 35S promoter (2x35S) and a Nos terminator (NOSt) sequence at the 5’ and 3’ end, respectively (Figure 2). For protein localization studies, the amplified AtCuAO2 and AtCuAO3 cDNAs, without and with a stop codon, respectively, were transferred from the pENTR/D-TOPO vector to the C-terminal and N-terminal YFP binary fusion vectors pEarlyGate101 or pEarlyGate104, respectively (AtCuAO2-YFP, YFP-AtCuAO3). AtCuAO1-YFP was obtained by transferring the AtCuAO1 coding region from AtCuAO1-pC-TAP to the pDONR221 vector, and from this to pEarlyGate101 using the Gateway recombination system. All vectors prepared were directly sequenced.

Protein expression in Nicotiana benthamianaand purification

Agrobacterium tumefaciens strain EHA105 cells were transformed with the AtCuAO1-pC-TAP, AtCuAO2-pC-TAP or AtCuAO3-pC-TAP plasmids using the freeze-thaw method and PCR confirmed.

A single Agrobacterium colony containing the construct of interest was cultured in liquid YEB medium overnight at 28°C with appropriate antibiotics. The bacteria were pelleted at 3 000 g for 20 min, resuspended in infiltration media (10 mM MES pH 5.7, 10 mM MgCl2 and 200 μM acetosyringone), adjusted to an OD600 of 0.5 and incubated at room temperature for at least 3 h. Agrobacterium cultures transformed with the tobacco etch potyvirus helper component protein (HC-Pro) silencing suppressor [53] were resuspended in infiltration media to the same OD600. Equal volume of cultures containing the construct of interest and HC-Pro were mixed and infiltrated into 4-week-old Nicotiana benthamiana plants using a 1 ml needleless syringe. Three days after infiltration, the leaves were collected and stored at −80°C.

For protein extraction and purification, the procedure described by [27] was followed with some modifications. Collected leaves were ground in liquid nitrogen and homogenized with one volume of buffer containing: 100 mM Tris–HCl pH 7.5, 150 mM NaCl, 10% glycerol, 0.1% TritonX-100, 1 mM PMSF and 1x complete protease inhibitor cocktail (Sigma, St. Louis, MO, USA). Homogenates were filtered through four layers of cheesecloth and centrifuged at 14 000 g for 10 min at 4°C. Protein concentration in the supernatant was determined by the Bradford assay (Bio-Rad, Hercules, CA, USA). The total protein extracts were incubated with IgG Sepharose 6 Fast Flow beads (Amersham Biosciences, Uppsala, Sweden) for 2 h at 4°C with gentle rotation. After centrifugation at 150 g for 3 min at 4°C, the IgG beads were recovered and washed three times with 10 ml of washing buffer (extraction buffer plus 350 mM NaCl). Elution from the IgG beads was performed by incubation with 12 μl (50 units) of 3C protease (Precision protease; Amersham Biosciences) in 5 ml of washing buffer at 4°C with gentle rotation overnight. Supernatants were recovered after centrifugation at 150 g for 3 min at 4°C and stored. The IgG beads were washed with 5 ml of washing buffer and centrifuged again. Supernatants were recovered and, after pooling the eluates, proteins were concentrated using an Amicon Ultra-15 Centrifugal Filter (Millipore Corporation, Billerica, MA, USA) and separated on 8% SDS-PAGE gel. Protein bands were visualized by immunoblotting using the α-myc antibody.

In Vitroactivity assay

The CuAO activity of the recombinant fusion-proteins (AtCuAO1-MYC9-His6, AtCuAO2-MYC9-His6, AtCuAO3-MYC9-His6) was assayed by measuring the formation of H2O2 by fluorometry using the Amplex-Red hydrogen peroxide assay according to the manufacturer’s instructions (Invitrogen Life Technologies). Thus, the purified fusion protein (1 μg), or the same volume of elution buffer as a control, was incubated with 1 mM of each substrate, namely Put, Spd or Spm, 50 μM Amplex Red reagent, and 0.1 U ml-1 horseradish peroxidase in 100 mM Tris–HCl buffer (pH 8.0), at 37°C for 1 h. Fluorescence was measured at 540 nm excitation and 590 nm emission with a SpectraMax M3 Multi-Mode Microplate Reader (Molecular Devices, Sunnyvale, CA, USA), using black 96-well plates (Costar, Corning Incorporated, USA). Correction for background fluorescence was made by subtracting the values of reaction medium without the substrate. Amine oxidase-inhibited reactions were pre-treated with 0.5 mM AG or 30 μM 8 HQL for 5 min at 30°C and then subjected to the assay procedure described above. All experiments were repeated three times

Protein localization analysis

A. tumefaciens strain EHA105 cells were transformed with the plasmids containing the fusion proteins AtCuAO1-YFP, AtCuAO2-YFP and YFP-AtCuAO3 and infiltrated into 3–4 week old N. benthamiana plants as described above.

For colocalization experiments, suspensions of A. tumefaciens harbouring the AtCuAO1-YFP expression construct were mixed with A. tumefaciens cultures harbouring constructs for expression of the red fluorescent protein (DsRed)-extracellular marker (Spg-DsRed) [32], while A. tumefaciens harbouring the AtCuAO2-YFP and YFP-AtCuAO3 expression constructs were mixed with bacteria cultures containing constructs for expression of the cyan fluorescent protein (CFP)-peroxisome marker (CFP-SKL). In both cases, A. tumefaciens cultures containing HC-Pro were added to the mixture in a ratio of 1:1:2 (v:v:v) of fusion protein:marker:HC-Pro to suppress silencing. Agroinfiltrated leaves were examined after 3–4 days by confocal laser-scanning microscopy using an Olympus FV1000 microscope (Olympus, Japan). We used the 515-, 405- and 595-nm laser to excite YFP, CFP and DsRed, respectively. Fluorescence was detected using an emission filter of a 530- to 630-nm band pass for YFP and DsRed and a 460- to 500-nm band pass for CFP. All images were acquired from single optical sections. Images were merged using the FV1000 Viewer software Ver.03.1 (Olympus, Japan).



Abscisic acid


1-aminocyclopropane-1-carboxylic acid


Aldehyde deshydrogenase




Amine oxidase




Betaine aldehyde deshydrogenase


Cooper-containing amine oxidase


γ-aminobutiric acid






Polyamine oxidase


Peroxisome targeting sequence




Salicylic acid






Tandem affinity purification.


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The authors thank Dr. M.D. Ludevid for the kind gift of extracellular marker Spg-DsRed, and the ABRC stock centre for the peroxisomal marker CFP-SKL and most of the vectors used in this work (pC-TAPa, pEarleyGate101, pEarleyGate104 and DKLAT1G62810). Authors are also grateful to Dr. R. Alcázar for critical reading of the manuscript. The excellent technical support from members of the Greenhouse and Microscopy facilities at CRAG is greatly appreciated. JPP was recipient of a PhD fellowship from CRAG. This work was supported by the Spanish Ministerio de Ciencia e Innovación [grant numbers BIO2008-05493-C02-01, CSD2007-00036 and BIO2011-29683] and the Generalitat de Catalunya [grant number SGR2009-1060].

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Correspondence to Teresa Altabella.

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Authors’ contributions

JP-P carried out the molecular genetic studies and the activity and localization assays, participated in the production of the recombinant proteins and in the design of the study, and helped to draft the manuscript. MG carried out the purification of the recombinant proteins. AFT participated in the design of the study and in the drafting of the manuscript. TA conceived of the study, participated in its design, performed the sequence alignment and drafted the manuscript. All the authors read and approved the final manuscript.

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Planas-Portell, J., Gallart, M., Tiburcio, A.F. et al. Copper-containing amine oxidases contribute to terminal polyamine oxidation in peroxisomes and apoplast of Arabidopsis thaliana. BMC Plant Biol 13, 109 (2013).

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