Skip to main content

Thank you for visiting You are using a browser version with limited support for CSS. To obtain the best experience, we recommend you use a more up to date browser (or turn off compatibility mode in Internet Explorer). In the meantime, to ensure continued support, we are displaying the site without styles and JavaScript.

Nitrogen represses haustoria formation through abscisic acid in the parasitic plant Phtheirospermum japonicum


Parasitic plants are globally prevalent pathogens that withdraw nutrients from their host plants using an organ known as the haustorium. The external environment including nutrient availability affects the extent of parasitism and to understand this phenomenon, we investigated the role of nutrients and found that nitrogen is sufficient to repress haustoria formation in the root parasite Phtheirospermum japonicum. Nitrogen increases levels of abscisic acid (ABA) in P. japonicum and prevents the activation of hundreds of genes including cell cycle and xylem development genes. Blocking ABA signaling overcomes nitrogen’s inhibitory effects indicating that nitrogen represses haustoria formation by increasing ABA. The effect of nitrogen appears more widespread since nitrogen also inhibits haustoria in the obligate root parasite Striga hermonthica. Together, our data show that nitrogen acts as a haustoria repressing factor and suggests a mechanism whereby parasitic plants use nitrogen availability in the external environment to regulate the extent of parasitism.


Parasitic plants make up ~1% of all angiosperm species, some of which are devastating agricultural weeds that cause major agricultural losses each year1,2,3. Parasitic plants range from obligate parasites that completely depend on their host for survival to facultative parasites that survive without a host but parasitize when conditions are suitable2,4. Despite differences in their lifestyle, all parasitic plants form an invasive organ termed the haustorium5 through which they penetrate the host and uptake water, nutrients, RNA, proteins, and hormones5,6,7,8,9,10.

Many parasitic plants, particularly the obligate parasites, require perception of host-exuded compounds such as strigolactones to initiate germination. Perception of a second host-derived compound, known as haustorium inducing factors (HIFs), initiates haustorium formation in both obligate and facultative parasites. The first identified HIF was 2,6-dimethoxy-1,4-benzoquinone (DMBQ), originally isolated from root extracts of infected sorghum plants11. DMBQ can induce early stages of haustoria formation even in the absence of a host11 in a wide range of parasitic plant species. In the facultative parasitic plant Phtheirospermum japonicum, perception of a nearby host via HIFs is followed by cell expansion and cell division at the haustorium initiation site, forming the characteristic swelling of the prehaustorium. Downstream signaling of HIFs requires reactive oxygen species (ROS) that accumulate in the haustorium after HIF perception12. Later, the developing haustorium attaches to the host and starts penetrating to reach the vascular cylinder of the host. Once the haustorium has reached the host’s vasculature, it starts forming a xylem connection between itself and the host known as the xylem bridge13,14,15,16. These series of events lead to the establishment of the mature haustorium.

Despite recent advances in our understanding of haustorium development, we know little about how environmental conditions affect plant parasitism. Nutrient availability is an important factor affecting plant parasitism. Infestations of the agriculturally devastating obligate parasite Striga are often associated with poor soil fertility17. Low soil fertility is thought to impede host defences and exacerbate the damaging effects of infection17. In addition, low nutrient levels in the soil, particularly phosphate, promotes host secretion of strigolactones which enhances Striga germination and infection levels. Improving soil fertility can reduce the production of germination stimulants while also improving host defences and host tolerance17,18,19,20,21. However, nutrients might also have effects on the parasite beyond germination. For instance, the application of certain nitrogen compounds reduces Striga shoot development22 whereas P. japonicum requires nutrient starvation to efficiently infect its hosts in vitro8,13,14 and high phosphorous inhibits Rhinanthus minor growth23. Together, these data suggest that nutrients might play a role beyond improving host fitness or reducing parasite development.

Nutrient availability affects many aspects of plant development including germination, root growth, shoot growth and flowering24,25,26. High nitrate levels generally promote shoot growth and repress root growth, in part, through the action of plant hormones. In Arabidopsis thaliana, rice, maize and barley, nitrates increase cytokinin levels which move to the shoot meristems to promote cell divisions and growth27,28,29,30,31. Nitrates also inhibit auxin transport and modify auxin response to promote root initiation but inhibit root elongation32. The hormone abscisic acid (ABA) too plays a role; nitrate treatments increase ABA levels in Arabidopsis root tips33 whereas ABA signaling is required for the inhibitory effects of high nitrates on root growth34. However, the mechanisms through which nutrient availability affects plant parasitism remain unknown.

Here, we show that nutrient-rich soils greatly reduce both root size and haustorial density in P. japonicum, and this effect is dependent specifically on nitrogen concentrations. Nitrogen application reduced ROS levels, blocked gene expression changes associated with haustoria formation and modified xylem patterning in the root. Nitrogen increased ABA levels and activated ABA responsive gene expression. Treating with ABA reduced haustoria initiation whereas inhibiting ABA biosynthesis or signaling reduced the inhibitory effect of nitrogen. Finally, we investigated the effects of nutrients in Striga hermonthica and found that similar to P. japonicum, nutrients decreased haustoria formation rates and infection rates, and this effect was specific to nitrogen and could be overcome by modifying phytohormone levels.


Nitrogen inhibits haustoria development

Previous work has demonstrated that nutrient-poor conditions are important for efficient Striga infestations and successful P. japonicum in vitro infections8,13,35,36. We tested whether successful P. japonicum-Arabidopsis infections in soil also required low nutrients by treating nutrient poor 50:50 soil:sand with or without fertilizer (51-10-43 N-P-K). P. japonicum shoot weights and heights were similar in both treatments, but root masses and haustorial density were higher under low nutrient conditions (Fig.1a–c; Supplementary Fig. 1a–c). To better understand the basis for reduced haustoria in high nutrient conditions, we grew 4–5-day old P. japonicum seedlings in vitro on water-agar or half-strength Murashige and Skoog medium (½MS)-agar (Supplementary Fig. 1d). Similar to fertilized soil, P. japonicum-Arabidopsis infections on ½MS-agar formed substantially fewer haustoria that also failed to form vascular connections with the host compared to those on water-agar (Fig.1d, e). To identify the compound(s) that caused haustoria arrest, we tested three of the major macroelements found in MS and tested one macroelement found in Gamborg’s B5 medium at similar concentrations as those found in ½MS or Gamborg’s medium. Agar media containing phosphate (KH2PO4 or NaH2PO4) or potassium (KH2PO4 or KCl) had little effect on haustoria formation, but agar media containing nitrogen including nitrates, ammonium or both (KNO3, NaNO3, NH4Cl, NH4NO3) inhibited P. japonicum-Arabidopsis infections and xylem bridge formation similar to ½MS (Fig.1d, e, i). Infections on ½MS lacking nitrogen did not affect haustoria formation, xylem bridge formation or anatomy (Fig.1d, e, i; Supplementary Fig. 1d–g) indicating that nitrogen was sufficient and necessary to block haustoria formation. Nitrogen application led to a reduction of haustoria and xylem bridge formation in a 50 μM to 20.6 mM range of concentrations (Fig.1f, g; Supplementary Fig. 1e–g). However, plate xylem length, area and xylem bridge number were unaffected in haustoria that formed xylem bridges regardless of nitrogen treatment (Fig.1e, Supplementary Fig. 1e–g). To test whether nitrogen blocked infection by acting on the parasite or host, we applied NH4NO3 or ½MS to P. japonicum growing alone in the presence of the haustoria inducting factor DMBQ. Adding DMBQ to water or ½MS lacking nitrogen resulted in similar numbers of prehaustoria, whereas adding DMBQ to NH4NO3 or ½MS greatly reduced prehaustoria formation (Fig. 1h, i) indicating the effect of nitrogen on haustoria initiation did not depend on host infection.

Fig. 1: Nitrogen inhibits P. japonicum haustoria formation.
figure 1

a, b Representative images and shoot and root fresh weight (FW) of P. japonicum during Arabidopsis infection with and without fertilizer (mean ± SD, n fertilizer= 11 plants, n water= 8 plants). c Haustoria numbers per cm2 P. japonicum root during Arabidopsis infection with and without fertilizer (mean ± SD, n fertilizer= 24 images analyzed, n water= 37 images analyzed). dg Haustoria numbers per P. japonicum seedling and xylem bridge formation percentage in in vitro Arabidopsis (Col-0) infections on ½MS (9 replicates), ½MS no N (2 replicates), 20.6 mM KNO3 (4 replicates), 10.3 mM NH4NO3 (5 replicates), 0.62 mM KH2PO4 (2 replicates), 1.9 mM NaH2PO4 (2 replicates), 10.3 mM NH4Cl (2 replicates), 10.3 mM NaNO3 (2 replicates), 10.3 mM KCl (2 replicates) or various NH4NO3 (2 replicates) concentrations (mean ± SD, n = 20 plants per treatment per replicate). h Prehaustoria numbers per P. japonicum seedling with 10 μM DMBQ and half-strength MS, half-strength MS no N or 10.3 mM NH4NO3 (mean ± SD, n = 10 plants per treatment, 3 replicates). i Representative images of P. japonicum haustoria during Arabidopsis in vitro infections with various nutrient treatments (replicates as indicated in (dg)). Scale bars 50 μm. b, c Asterisks represent *P < 0.05, **P < 0.001, ***P < 0.0001, Student’s t test, two tailed. Comparisons to the water treatment. dh Different letters represent P < 0.05, one-way ANOVA followed by Tukey’s HSD test. Source data provided.

Haustoria formation induces widespread transcriptional changes

To investigate how nitrogen availability affected haustoria formation in P. japonicum, we performed a time course RNAseq experiment of P. japonicum infecting Arabidopsis Col-0 in vitro on agar plates treated with water or 10.3 mM NH4NO3. We also included a treatment with 0.08 μM 6-benzylaminopurine (BA), a synthetic cytokinin, to test for similarities between NH4NO3 and BA transcriptional responses since previous studies have found that nitrogen treatments increase cytokinin levels in Arabidopsis, rice, maize and barley27,28,29,30. P. japonicum and Arabidopsis were physically aligned at time 0 to synchronize infections (Supplementary Fig. 1d) and tissues surrounding the root tips where haustoria normally emerge were collected at 0,12, 24, 48, 72 h post-infection (hpi) for the water treatment and 0,12, 24 hpi for the NH4NO3 and BA treatments (Fig. 2a). Additionally, as a control to distinguish transcriptional changes specific to haustorium formation, we included P. japonicum that grew without a host on agar plates containing water, NH4NO3 or BA (Fig. 2a). As observed previously (Fig. 1), P. japonicum treated with NH4NO3 formed few to no prehaustoria whereas the water treatment resulted in successful haustoria formation. With the water treatment, we observed an increasing number of differentially expressed genes in infected samples compared to control samples as time progressed (Supplementary Fig. 2a). Co-expression analyses enabled us to classify genes into 8 clusters with distinct expression patterns during haustorium formation (Fig. 2b, Supplementary Fig. 2b, Supplementary Data 1). Cluster 2, 3 and 8 whose gene expression peaked at early stages of haustoria formation (12 and 24hpi) had an over representation of genes that belong to Gene Ontology enrichment (GO) categories related to transcription, translation, signaling processes and cell expansion/replication (Supplementary Fig. 3). Cluster 4, 5, and 7 whose gene expression peaked at later time points in haustorium formation (48 and 72hpi) had an over representation of genes that belong to GO categories related to response to oxidative stress, cytokinin metabolic process, fatty acid biosynthetic process, lignin, sucrose and carbohydrate metabolism (Supplementary Fig. 3). We looked at the expression of individual genes in our transcriptome and identified an upregulation of P. japonicum auxin-related YUCCA3 (PjYUC3), LIKE AUXIN RESISTANT 1 (PjLAX1), PIN-FORMED 9 (PjPIN9), and cambium-related WUSCHEL RELATED HOMEOBOX 4 (PjWOX4), genes whose expression has been previously observed to increase during P. japonicum infections14,15,37 (Fig. 2c). Genes associated with cytokinin metabolism such as P. japonicum CYTOKININ OXIDASE 3 (PjCKX3), CYTOKININ OXIDASE 1 (PjCKX1), LONELY GUY 8 (PjLOG8), cell wall remodeling such as PECTIN METHYLESTERASE INHIBITOR 9 (PjPMEI9), cell cycle such as CYCLIN A (PjCYCA) and ROS related such as PEROXIDASE 33 (PjPRX33) were upregulated as well (Fig. 2c) indicating substantial transcriptional reprogramming as the haustoria formed.

Fig. 2: Transcriptomic changes during haustorium formation.
figure 2

a Illustration describing the set-up for the RNAseq experiment. P. japonicum and Arabidopsis (infect) or P. japonicum alone (control) were placed on media containing water, 10.3 mM NH4NO3 or 0.08 μM BA; 3–4 mm of root tip or haustorium formation area was harvested at 0, 12, 24, 48, 72 hpi time points for the water treatment and 0, 12, 24 hpi time points for the NH4NO3 and BA treatments. b Clustering of differentially expressed genes in the water infect treatment based on their co-expression patterns over five time points; numbers in parentheses represent the number of genes in the cluster. c Normalized P. japonicum counts of PjYUC3, PjLAX1, PjPIN9, PjWOX4, PjPMEI9, PjCKX1, PjCKX3, PjLOG8, PjCYCA, PjPRX33 over 5 time points in the water infect treatment (mean ± SD, n = 3 libraries).

Nitrogen inhibits genes associated with early haustorial development

Nitrogen prevented haustoria formation (Fig. 1) so we looked at when this block occurs transcriptionally. We compared the transcriptional differences between infections on water and infections on NH4NO3 and found between 4000 and 6000 genes were expressed differently between treatments at each time point (Supplementary Fig. 2c–h) including PjYUC3, PjWOX4, and PjPMEI9 whose expression was upregulated during successful haustoria formation on the water treatment but were not activated in the NH4NO3 treatment (Fig. 3a, b). Moreover, NH4NO3 treatment reduced the expression levels of cell cycle and ROS related genes (Fig. 4a, b). We tested this observation further and found EdU staining for cell division decreased (Fig. 4c) whereas dihydroethidium (DHE) and 2′,7′-dichlorodihydrofluorescein diacetate (H2DCFDA) staining for ROS accumulation reduced at the haustorium formation site at 24 hpi of NH4NO3 treatment (Fig. 4d–g) consistent with nitrogen acting early to block haustoria induction (Fig.1). We next compared NH4NO3 infect with NH4NO3 control and found fewer than 70 differentially expressed genes at any time point (Supplementary Fig. 2c) suggesting that very few infection-specific genes were upregulated in NH4NO3 infections. Consistent with this, less than 20 of these genes at each time point were also differentially expressed during water infections. Finally, we compared the NH4NO3 control to water control datasets to see which genes prior to infection might influence haustoria induction. We found a GO enrichment for cell wall and lignin-related genes downregulated in the NH4NO3 control compared to the water control (Supplementary Fig. 4a). Genes downregulated included xylem-related P. japonicum XYLEM CYSTEINE PEPTIDASE 1 (PjXCP1), LACCASE 11 (PjLAC11), IRREGULAR XYLEM 3 (PjIRX3), CELLULOSE SYNTHASE A4 (PjCESA4), PEROXIDASE 66 (PjPRX66), quinone perception related genes CANNOT RESPOND TO DMBQ LIKE 2 (PjCADL2) and CANNOT RESPOND TO DMBQ LIKE 4 (PjCADL4)38 and ROS related genes PEROXIDASE 33 (PjPRX33) and PEROXIDASE 25 (PjPRX25) (Fig. 3b, Supplementary Fig. 2i). Cytokinin-related GOs were also enriched in the genes downregulated by nitrogen (Supplementary Fig. 4a) and we found no substantial overlap between differentially expressed genes in the BA control and NH4NO3 control samples (Supplementary Fig. 5a). Together, these data suggested that nitrogen blocked the infection process at an early stage and nitrogen did not induce a substantial cytokinin response in P. japonicum.

Fig. 3: NH4NO3 treatment modifies P. japonicum gene expression.
figure 3

a Heatmap of 300 P. japonicum genes with the highest log2 expression fold change during haustoria formation over three time points in the water infect vs water control and NH4NO3 infect vs water infect. b Normalized P. japonicum counts of PjYUC3, PjWOX4, PjPMEI9, PjXCP1, PjCADL4, PjPRX66 over three time points shown for control and infect in the NH4NO3 and water treatments (mean ± SD, n = 3 libraries).

Fig. 4: NH4NO3 reduces ROS accumulation and cell division in P. japonicum.
figure 4

a Heatmap of 27 cell cycle and 30 ROS related P. japonicum genes in NH4NO3 infect compared to water infect RNAseq datasets. b Normalized P. japonicum counts of PjCYCA, PjCYCD, PjPRX33, PjPRX25 over three time points shown for control and infect in the NH4NO3 and water treatment, bars represent mean ± SD. c, d, g Representative images of P. japonicum in vitro Arabidopsis Col-0 infections with water or 10.3 mM NH4NO3 at 0, 2 and 24 h post-infection (hpi) stained with EdU (c), dihydroethidium (DHE) (d) or 2′,7′-dichlorodihydrofluorescein diacetate (H2DCFDA) (n = 20 plants per treatment per replicate, 2 replicates). Scale bars 100 μm. e, f DHE at 0 and 24 hpi (n = 22, water 0 hpi n = 17) and H2DCFDA at 0, 2, 24 hpi (n = 12, 24 hpi water treatment n = 6) intensity in the P. japonicum haustorium formation area after water infect or NH4NO3 infect (mean ± SD; Comparisons to water treatments. Asterisks represent *P < 0.05, **P < 0.001, ***P < 0.0001, Student’s t test, two tailed). Source data provided.

Nitrogen increases ABA levels in P. japonicum

To further investigate how nitrogen arrests haustoria formation, we performed hormonal profiling on P. japonicum seedlings or mature roots infecting Arabidopsis with and without nitrogen treatment. In the parasite, levels of the active cytokinin trans-zeatin (tZ) and the cytokinin precursor trans-zeatin riboside (tZR) increased in successful infections, whereas in the host, levels of tZ and tZR increased in the presence of nitrates or successful infections, similar to previous studies8,27,28,29,31 (Fig. 5a, Supplementary Fig. 6a, b). Neither jasmonic acid (JA), indole acetic acid (IAA), gibberellic acid (GA) A1, ABA nor salicylic acid (SA) were substantially induced in the parasite by infection (Fig. 5a, b, Supplementary Fig. 6a, b). However, ABA and SA were significantly increased by NH4NO3 treatments in 50-day-old P. japonicum control and infect roots compared to water alone (Fig. 5b). In 20-day-old P. japonicum whole seedlings, ABA levels also increased in both infect and control NH4NO3 treated P. japonicum seedlings compared to water treatments (Fig. 5a). In the Arabidopsis host, ABA levels were also increased both by nitrogen treatments and by P. japonicum infection (Fig. 5a). This increase was dependent on host ABA biosynthesis since the increase was blocked in the ABA biosynthesis mutant aba deficient 2-1 (aba2-1) (Fig. 5a). Cytokinin moves from P. japonicum to Arabidopsis during infections8 but we found no evidence that ABA moved from parasite to host since Arabidopsis ABA levels in aba2-1 infections were similar to not infected aba2-1 plants (Fig. 5a). However, P. japonicum ABA levels were reduced in aba2-1 infections compared to Col-0 infections, perhaps from reduced movement of host-derived ABA to the parasite or from the host reducing parasite ABA signaling or biosynthesis. We looked at our transcriptome analysis and found that P. japonicum genes homologous to Arabidopsis ABA responsive genes had increased expression levels in the NH4NO3 treatment compared to the water treatment for both infect and control tissues (Fig. 5c, Supplementary Fig. 4b, Supplementary Fig. 5e). This expression pattern was not seen for the same genes when comparing the BA control to water control, BA infect to water infect, or water infect to water control samples (Supplementary Fig. 4c, Supplementary Fig. 5b, f, g) suggesting the increased ABA response was specific to NH4NO3 treatment. Most cytokinin-related genes were not differentially expressed in the NH4NO3 infect compared to the water infect or NH4NO3 control compared to water control treatments—with some exceptions—further supporting our finding that NH4NO3 treatment in P. japonicum induces an ABA response rather than a cytokinin response (Fig. 5d, Supplementary Fig. 4d, e). However, cytokinin-related genes were differentially expressed during later time points in water infect compared to water control samples (Supplementary Fig. 5h), implicating cytokinin response in later haustorium development. To see whether the P. japonicum genes homologous to Arabidopsis ABA responsive genes were ABA responsive, we selected four upregulated genes in our NH4NO3 control RNAseq dataset and found by qPCR that transcript levels of three of them were significantly increased by exogenous ABA (Supplementary Fig. 5c). We tested the expression levels of these genes and one ABA biosynthesis homolog, PjABA2, in P. japonicum grown on various soil:sand ratios and found that the expression levels of FRUCTOSE-BISPHOSPHATE ALDOLASE 2 (PjFBA2), ABA INSENSITIVE 1 (PjABI) and PjABA2 were lower in P. japonicum roots in nutrient poor soils (Supplementary Fig. 5d), suggesting that some ABA responses and ABA biosynthesis were downregulated in plants grown in nutrient poor soils, and conversely, upregulated in nutrient-rich soils (Supplementary Fig. 5d). SA levels also increased during nitrogen treatment in the parasite (Fig. 5a,b) but most P. japonicum genes homologous to Arabidopsis SA-responsive genes were not differentially expressed in the NH4NO3 infect compared to the water infect treatment (Supplementary Fig. 5i). Together, these data suggest that nitrogen increased ABA levels and induced ABA responses in P. japonicum.

Fig. 5: ABA levels increase during nitrogen treatment.
figure 5

a Hormonal quantification of salicylic acid (SA), jasmonic acid (JA), abscisic acid (ABA), indole acetic acid (IAA), trans-zeatin (tZ) and trans-zeatin riboside (tZR) in P. japonicum whole seedlings and Arabidopsis (Col-0, aba2-1) whole seedlings treated with 10.3 mM NH4NO3 (mean ± SD, n = 4 plants per treatment, 4 replicates). b Hormonal quantification of SA, JA, ABA, and IAA in P. japonicum mature roots treated with 10.3 mM NH4NO3 (mean ± SD, n = 4 roots per treatment, 4 replicates). c Heatmap of the log2 fold change of 629 genes homologous to Arabidopsis ABA responsive genes (up or downregulated) for three time points in the NH4NO3 infected vs the water infected RNAseq dataset in P. japonicum. d Heatmap of the log2 fold change of 67 genes homologous to Arabidopsis cytokinin responsive genes (up or downregulated) for three time points in the NH4NO3 infect vs the water infect RNAseq dataset in P. japonicum. a, b Comparisons to respective control samples. Asterisks represent *P < 0.05, **P < 0.001, ***P < 0.0001, Student’s t test, two tailed. Source data provided.

ABA affects haustoria formation

To investigate the role of ABA on haustorium formation in P. japonicum, we applied ABA exogenously using in vitro infection assays. ABA treated plants formed less haustoria than water treated plants (Fig. 6a, b). The application of fluridone, a chemical inhibitor of ABA biosynthesis, significantly reduced xylem bridge formation but did not affect haustoria formation (Fig. 6a–c). We reasoned that if nitrogen induced ABA to repress haustoria, we could overcome the inhibitory effects of nitrogen by blocking ABA biosynthesis with fluridone. Indeed, treating ½MS with fluridone increased haustoria numbers compared to ½MS alone but they remained intermediate to the water treatment (Fig. 6a–c). As a second approach, we used the Arabidopsis abi1-1 dominant mutant that represses ABA signaling in Arabidopsis and when expressed in Nicotiana39,40. We found that haustoria formation in non-transgenic hairy roots was suppressed by nitrogen but when we overexpressed Atabi1-1 in P. japonicum, haustoria formation was unaffected by the presence of nitrogen (Fig. 6d–f). These results demonstrated that blocking ABA signaling in P. japonicum roots was sufficient to rescue the suppressive effects of nitrogen. We investigated host ABA pathways but P. japonicum infecting Arabidopsis aba2-1 or aba1-1C did not have differences in haustoria and xylem bridge formation, suggesting that altering host ABA biosynthesis or signaling did not affect parasitism (Supplementary Fig. 6c, d). SA levels were also induced by NH4NO3 in P. japonicum and Arabidopsis (Fig. 5a, b, Supplementary Fig. 6a) so we tested the exogenous application of SA and found it decreased haustorial numbers but did not affect xylem bridge formation (Supplementary Fig. 6e–g, j, k). Thus, SA might act as a second signal to regulate haustoria, however, SA related genes were not differentially expressed by NH4NO3 treatment (Supplementary Fig. 5i) suggesting nitrogen does not induce an SA response.

Fig. 6: ABA represses P. japonicum haustoria formation.
figure 6

a, b Haustoria number per P. japonicum seedling and xylem bridge formation percentage in in vitro Arabidopsis (Col-0) infections treated with ABA (6 replicates), fluridone (Fl) (6 replicates), ½MS (6 replicates), ½MS no N (6 replicates) or ½MS + fluridone (5 replicates) (mean ± SD, n = 20 plants per treatment per replicate). c Representative images of P. japonicum haustoria during Arabidopsis in vitro infection with ABA, fluridone, ½MS or ½MS + fluridone. Scale bars 50 μm. 5 replicates. d Haustoria number per P. japonicum hairy roots overexpressing Atabi1-1 in in vitro infection assay with Arabidopsis Col-0 and ½MS or ½MS no N (mean ± SD, pMAS::Atabi1-1 n = 19 for ½MS and n = 24 for ½MS no N treatments, non-transgenic n = 30 for ½MS and n = 29 for ½MS no N treatments). e Expression levels of Atabi1-1 in fluorescent and non-fluorescent hairy roots analyzed by qPCR (mean ± SD, n = 3 roots per treatment, 3 replicates). f Representative images of P. japonicum hairy roots in the ½MS no N treatment in brightfield and red fluorescence fields, the haustorium (H) is denoted by an arrow, scale bars 500 μm. 3 replicates. a, b, d Different letters represent P < 0.05, one-way ANOVA followed by Tukey’s HSD test. e Asterisks represent *P < 0.05, **P < 0.001, ***P < 0.0001 compared to ½MS transgenic roots, Student’s t test, two tailed. Source data provided.

Since ABA is important for various developmental processes including xylem formation41, we analyzed the P. japonicum transcriptome in water infect compared to water control treatments and found that some P. japonicum genes homologous to Arabidopsis ABA responsive genes increased expression late during infection indicating they might have a relevant role during later stages of haustoria formation such as xylem bridge formation (Supplementary Fig. 5g). Exogenous ABA treatments did not increase xylem bridge formation, numbers or size (Fig. 6b, c, Supplementary Fig. 6e–i) but treatment with fluridone blocked xylem bridge formation (Fig. 6b, Supplementary Fig. 6i). Exogenous ABA application to P. japonicum was previously shown to enhance the number of differentiating xylem strands in primary root tips41. We repeated this assay but used nitrogen treatments on P. japonicum seedlings. ABA, NH4NO3 and ½MS all had a similar phenotype of increased xylem strand differentiation compared to water-only treatments (Supplementary Fig. 6l). These data showed that ABA treatment could phenocopy nitrogen treatment and that ABA played additional roles in both xylem bridge formation and also in modulating xylem patterning in response to nitrogen levels.

Nitrogen affects Striga infection rates

Previous field studies have shown that Striga infestation is decreased after nitrate application18,42. We investigated the effect of nutrients upon S. hermonthica using in vitro infection assays with rice as the host. In the presence of NH4NO3, KNO3, KH2PO4, or NaH2PO4, Striga infection rates were not significantly decreased 2 weeks after infection (Fig. 7a). However, 4 weeks after infection nitrogen application lead to a significant decrease in the percentage of Striga that infected its rice host and formed more than three leaves (Fig. 7a, d). Striga development was also hindered in the presence of nitrogen where the appearance of plants with 3–5 leaf pairs and more than 6 leaf pairs were decreased compared to the water treatment (Supplementary Fig. 7a). We tested whether this effect was due to improved host fitness or reduced Striga infectivity by treating Striga with DMBQ in the presence of nitrogen. Prehaustoria formation by DMBQ was significantly reduced in the presence of NH4NO3, NH4Cl, or KNO3 (Fig. 7b, c, Supplementary Fig. 7b) demonstrating that, like P. japonicum, early Striga haustoria formation is inhibited by high nitrogen. Striga is highly ABA43 resistant, but nonetheless we tested exogenous application of ABA or fluridone and found they did not have an effect on Striga haustoria formation in the presence or absence of nitrogen (Fig. 7e, Supplementary Fig. 7c, d). Auxin biosynthesis is important for haustoria formation14 and we found that auxin-related genes were upregulated during Striga-rice infection indicating a possible role for auxin in promoting Striga haustoria formation (Fig. 7f). We applied exogenous auxin to nitrogen-grown Striga and found it could overcome the inhibitory effects of nitrogen (Fig. 7g), suggesting a role for auxin acting downstream of nitrogen. Exogenous auxin treatment did not affect haustoria formation in P. japonicum and did not rescue the haustoria inhibitory effect of ABA or ½MS (Supplementary Fig. 7e, f) consistent with P. japonicum and Striga using different hormone signaling pathways for nitrogen inhibition.

Fig. 7: Nitrogen inhibits Striga infection rates.
figure 7

a Striga infection rate of rice at 2 and 4 weeks with 20.6 mM KNO3, 10.3 mM NH4NO3, 0.62 mM KH2PO4 or 1.9 mM NaH2PO4 (mean ± SD, n = 8 plants per treatment, 3 replicates). b Effect of 10.3 mM NH4NO3 on Striga prehaustorium formation induced by 10 μM DMBQ (mean ± SD, n = 8 per treatment, 3 replicates). c Effect of 10.3 mM NH4NO3, 10.3 mM NH4Cl and 29.5 mM KNO3 on Striga prehaustorium formation induced by 10 μM DMBQ (mean ± SD, n = 8 plants per treatment, 3 replicates). (d) Representative images of Striga infecting rice at 2 weeks after infection. Scale bars 1 mm. 3 replicates. e, g Effect of 10 μM ABA, 10 μM fluridone, 5 mM NH4NO3, 5 mM NH4NO3 + 10 μM fluridone, 500 nM NAA, 500 nM IAA, 10.3 mM NH4NO3, 10.3 mM NH4Cl or 29.5 mM KNO3 on Striga prehaustorium induction by 1 (e) or 10 (g) μM DMBQ (mean ± SD, n = 8 plants per treatment, 3 replicates). f Heatmap of Striga auxin-related gene expression during rice infection. h Graphical representation of a putative model of nitrate-ABA mediated haustoria regulation. a, b, e Different letters represent P < 0.05, one-way ANOVA followed by Tukey’s HSD test. c, g Asterisks represent *P < 0.05, **P < 0.001, ***P < 0.0001 compared to water treatments, Student’s t test, two tailed. Source data provided.


Here, we describe a mechanism whereby external nitrogen levels regulate haustoria formation in the facultative root parasite P. japonicum (Fig. 7h). This effect did not occur with phosphate or potassium and instead appeared highly specific to nitrogen in micromolar concentrations (Fig. 1f, g). A previous study showed that increased nitrogen supply to Medicago sativa also reduced P. japonicum parasitism44, consistent with our results. We propose that local nitrogen supply at the site of infection has a suppressive effect upon the parasite in addition to nitrogen’s proposed roles to stimulate host defenses and reduce host HIF production. Striga haustoria formation and infection rates were also inhibited by nitrogen (Fig. 7a–c) which is consistent with previous observations that external nitrogen reduces Striga growth22,42. However, our results point to an earlier additional role for nitrogen by preventing haustoria to develop beyond an initial swell (Fig.1h, Supplementary Fig. 7b). DHE and H2DCFDA staining revealed nitrogen reduced ROS levels in P. japonicum roots prior to infection (Fig. 4), whereas quinone perception related genes PjCADL2 and PjCADL4 were downregulated by nitrogen which all could negatively affect HIF perception or downstream HIF signaling12. Alternatively, starvation could increase ROS and PjCADL levels to induce competency for HIF perception and haustoria elongation. As such, the observed reduction in Striga infestations in nutrient-rich fields18 could be from a combination of reduced host germination stimulant production and our findings that nitrogen reduced haustoria formation and Striga growth. Our results also suggest a conserved role for nitrogen acting as a haustoria repressing factor in both facultative and obligate Orobanchaceae family members.

Beyond parasitism, nitrogen has strong effects upon plant root architecture and organogenesis. In Arabidopsis, mild nitrogen deficiency enhances lateral root elongation, whereas uniform high nitrogen levels repress lateral root development45,46,47. In nodulating plants, high nitrogen levels in the environment repress nodule formation in Medicago truncatula, soybean and alfalfa through a regulatory mechanism involving multiple hormones and peptides48,49,50,51,52. Our data and these previous findings suggest a common regulatory theme whereby low nitrogen levels promote organ growth to uptake additional nutrients, whereas high nitrogen levels repress organ growth to avoid unnecessary resources spent on nutrient acquisition.

In species like Arabidopsis, maize, rice and barley, high nitrates increase cytokinin levels and these are important for root development and shoot growth27,28,29,30. We found host and parasite cytokinin levels were strongly induced by infection (Fig. 5a, Supplementary Fig. 6a), consistent with previous findings8, but nitrogen itself did not increase tZ levels, tZR levels or induced a strong cytokinin response in young P. japonicum and had a mixed effect in mature P. japonicum where tZ levels increased but tZR levels decreased upon nitrate treatment (Supplementary Fig. 6b). Notably, a recent study found that nitrogen treatment of Lotus japonicus inhibited cytokinin biosynthesis, reduced cytokinin levels and reduced nodule formation53. We saw a similar situation in young P. japonicum since nitrogen treatment reduced trans-zeatin levels and did not induce a strong cytokinin response (Fig. 5a, d). Thus, both P. japonicum and Lotus appear to increase cytokinin levels in response to successful haustoria or nodule formation8,54 yet do not necessarily increase cytokinin in response to high nitrogen. This situation differs from many other flowering plants and might be a convergent strategy to use cytokinin to signal successful symbiosis rather than nutrient abundance.

ABA plays an important role in parasitic plants and we observed that nitrogen increased ABA levels in P. japonicum independently of infection, while P. japonicum infection increased ABA levels in Arabidopsis (Fig. 5a). ABA levels are known to increase in both Rhinanthus minor and Cuscuta japonica, as well as their hosts, after infection55,56. Striga parasitism also increases host ABA levels in tomato and maize, and commonly induces symptoms in the host mimicking drought stress57,58. The increase in ABA we observed in the host Arabidopsis was likely due to a stress or defense response rather than movement from the parasite, however, increases in ABA levels in the parasite may have come in part from the host. Such ABA increases in the parasite appeared biologically relevant since treatments with exogenous ABA reduced haustoria numbers whereas perturbing ABA biosynthesis or ABA signaling in P. japonicum chemically or genetically overcame nitrogen inhibition (Fig. 6). These results suggest that nitrogen regulated haustoria formation in part via increasing ABA levels and ABA response which in turn repressed early stages of haustoria development including cell division. Striga and Cuscuta are highly insensitive to ABA43,59 and Striga did not respond to ABA in our assays (Fig. 7, Supplementary Fig. 7), indicating that these species likely use additional mechanisms for nitrogen-induced haustoria repression such as modifying auxin response which differed from the situation in P. japonicum (Supplementary Fig. 7e, f). Other factors including SA or proteins known to affect lateral root or nodule formation likely also play a role in haustoria regulation.

Our assays revealed several developmental roles for ABA in P. japonicum. ABA was important for haustoria inhibition and ABA treatment produced haustoria that were underdeveloped or did not attach well, likely explaining the partial reduction in xylem bridge formation from ABA treatment (Fig. 6). ABA was also important for xylem development since chemical inhibition of ABA biosynthesis led to reduced xylem bridge formation whereas nitrogen and ABA treatments induced early xylem differentiation in the primary root tip (Fig. 6b, Supplementary Fig. 6l). However, nitrogen also reduced the expression of xylem-related genes in the haustoria and surrounding tissues (Fig. 3, Supplementary Fig. 2) which might relate to differing roles for ABA both promoting xylem differentiation but also inhibiting haustoria formation.

In nodulating plants, such as Lotus japonicus, Trifolium repens and Medicago truncatula, ABA acts as a negative regulator of nodules by repressing nod factor signaling and cytokinin responses60,61,62. Exogenous application of ABA blocks the early stages of infection in Lotus japonicus61, similar to the situation we observe with haustoria in P. japonicum. We propose that at least some parasitic plants and legumes share another common regulatory theme whereby ABA inhibits symbiotic organ formation. However, more work will be required to investigate these parallels including whether nitrogen induces ABA in legumes and whether ABA inhibits HIF signaling in parasitic plants. Given that legumes and most parasitic plants are distantly related, it begs the question of whether such ABA and cytokinin regulatory features might be an important adaptation for symbiotic nutrient acquisition.


Plant materials and growth conditions

P. japonicum (Thunb.) Kanitz ecotype Okayama seeds harvested in Okayama and Karuizawa, Japan were used for our experiments63. Arabidopsis ecotype Columbia (Col-0) accession was used as Arabidopsis wild-type (WT). Arabidopsis aba2-1 and abi1-1C were published previously64,65. For in vitro germination, seeds were surface sterilized with 70% (v/v) EtOH for 20 min followed by 95%(v/v) EtOH for 5 min then left to air-dry to remove remaining EtOH. The seeds were then sown on petri dishes containing ½MS medium (0.8% (w/v) plant agar, 1% (w/v) sucrose, pH 5.8). After overnight stratification in the dark and 4 oC, the plants were transferred to 25 oC long-day conditions (16-h light:8-h dark and light levels 100 μmol m−2 s−1).

Striga hermonthica (Del.) Benth seeds were kind gifts provided by Dr A. G. T. Babiker (Environment and Natural Resources and Desertification Research Institute, Sudan). Rice seeds (Oryza sativa L. subspecies japonica, cvs Koshihikari) used in this study were originally obtained from National Institute of Biological Sciences (Tsukuba, Japan) and propagated in the Yoshida laboratory. The Striga hermonthica seeds were sterilized with a 20% (v/v) commercial bleach solution for 5 min and washed thoroughly with sterilized water on a clean bench. After that, these surface-sterilized Striga seed were placed in 9 cm petri dishes with moisturized glass fiber filter paper (Whatman GF/A) and conditioned at 25 oC in the dark for 7 days. The conditioned Striga seeds were treated with 10 nM Strigol66 for 2 hours prior to rice-infection treatments. For haustorium induction assays, the conditioned Striga seeds were treated with 10 nM Strigol at 25 oC for 1 day in the dark before starting incubation in various nutrient media with or without DMBQ and hormones for 24 h in dark condition.

Rice seeds were de-husked and sterilized with a 20% (v/v) commercial bleach solution (Kao Ltd., Japan) for 30 min with gentle agitation. The rice seeds were then washed thoroughly with distilled water and placed on filter papers in 9 cm petri dishes filled with 15 mL sterilized water in a 16-h light/8-h dark cycle at 26 oC for 1 week.

In vitro infection assays with P. japonicum

Four to five days old P. japonicum seedlings were transferred for three days to nutrient-free 0.8% (w/v) agar medium or 0.8% (w/v) agar medium supplemented by nutrient or hormone treatment: ½MS, ½MS no N, 20.6 mM KNO3, 50 μM-20.6 mM NH4NO3, 0.62 mM KH2PO4, 1.9 mM NaH2PO4, 10.3 mM NH4Cl, 20.6 mM NaNO3, 5 μM ABA, 10 μM Fluridone, 5 μM SA, 500 nM NAA, or 10.3 mM KCl. Five days old Arabidopsis seedling were aligned next to and roots place in contact with these pre-treated P. japonicum roots for infection assays. Haustorium formation and xylem bridge development were measured at seven days post infection using a Zeiss Axioscope A1 microscope. In vitro infection assays where a host was present were labeled as “infect” regardless of whether a successful infection occurred between host and parasite. Control assays where no host was added were labeled as “control”. In these experiments 20 plants per sample were used and the experiments were replicated at least twice.

Haustorium induction assay

Four to five days old P. japonicum seedlings were transferred to nutrient-free 0.8% (w/v) agar medium or 0.8% (w/v) agar medium supplemented by nutrients (½MS, ½MS no N, NH4NO3) for a three days pre-treatment. Subsequently, seedlings were transferred to 0.8% (w/v) agar medium containing DMBQ (Sigma-Aldrich) or DMBQ with or without nutrient treatment and grown vertically for four to five days for haustorium induction. In these experiments 20 plants per sample were used and the experiments were replicated at least twice.

Greenhouse experiments

Ten days old P. japonicum seedlings were germinated in vitro as described above. The seedlings were then transferred to pots with 50:50 soil:sand ratio. Arabidopsis seeds were sprinkled around the P. japonicum seedling. The pots were placed at 25 oC and long-day conditions (16-h light:8-h dark and 100 μmol m−2 s−1) and 60% humidity for 1.5 months. During this time the plants were given deionized water or water supplemented with fertilizer (commercial fertilizer Blömstra 51-10-43 N-P-K at 2 ml/L). Eight to fifteen plants per sample were used and this experiment was replicated three times.

Histological staining

Dissected P. japonicum roots or P. japonicum roots infecting A. thaliana were fixed in ethanol-acetic acid (75%/25%) solution under vacuum infiltration for 5 min. Then stained with Safranin-O solution (0.1%) at 90oC for 5 min. The root tissue was then cleared in chloral hydrate solution (chloral hydrate: glycerol: water 8:1:2) for two to three days before observation with a Zeiss Axioscope A1 microscope13.

EdU and ROS staining

Five days old P. japonicum seedlings were treated with water or 10.3 mM NH4NO3 for three days before host addition (Arabidopsis Col-0). 20 plants per sample were collected at 0 and 24 hpi, these experiments were replicated twice. EdU (Click-iT™ EdU Cell Proliferation Kit, Invitrogen) staining was used for the estimation of cell division. Briefly, P. japonicum roots were incubated in 10 μM EdU for 30 min at 25 oC followed by tissue fixation and permeabilization following the manufacturer’s instructions. EdU detection was performed with confocal microscopy (Zeiss LSM780).

For hydrogen peroxide staining 2′,7′-dichlorodihydrofluorescein diacetate CM-H2DCFDA (excitation/emission 492 nm/517 nm; ThermoFisherTM, C6827) was used and for superoxide staining dihydroethidium (DHE) (excitation/emission 510 nm/595 nm; Sigma-Aldrich, D7008) staining was used, P. japonicum roots were incubated in 10 μM CM-H2DCFDA or 30 μM DHE solution in 50 mM PBS for 30 min in the dark with gentle shaking, followed by three times washing with 50 mM PBS. CM-H2DCFDA or DHE detection was performed using confocal microscopy (Zeiss LSM780). Fluorescent intensity measurements were taken using ImageJ.

Xylem strand measurement

Five days old P. japonicum seedlings (n = 19) were treated with 1 μM ABA or 5 μM ABA, ½MS no N, ½MS or 5 mM NH4NO3 for three days. Afterwards, the number of xylem strands were measured at 2 mm from the root tip with a Zeiss Axioscope A1 microscope.

Sample preparation for RNAseq

40 four to five days old P. japonicum seedlings were transferred to nutrient-free 0.8% (w/v) agar medium or 0.8% (w/v) agar medium supplemented with 10.3 mM NH4NO3 or 0.08 μM BA for 3 days prior to infection with Arabidopsis Col-0. As a control group, 40 P. japonicum seedlings per treatment (water, 10.3 mM NH4NO3 or 0.08 μM BA) remained without the Arabidopsis host. For the water treatment infect and control samples, five time points were prepared (0,12, 24, 48, 72 hpi). For the NH4NO3 and BA treatments, infect and control samples were prepared for three time points (0, 12, 24 hpi). One to two mm from P. japonicum and Arabidopsis root tips were harvested for the control plants and the 0 hpi infect plants. For the 12, 24, 48, 72 hpi time points, the haustorium, including 1–2 mm above and below tissue was collected together with the corresponding region of the Arabidopsis root. Three biological replicates were prepared for this experiment. RNA extraction was performed using the ROTI®Prep RNA MINI (Roth) kit following the manufacturer’s instructions. The isolation of mRNA and library preparation were performed using NEBNext® Poly(A) mRNA Magnetic Isolation Module (#E7490), NEBNext® Ultra™ RNA Library Prep Kit for Illumina® (# E7530L), NEBNext® Multiplex Oligos for Illumina® (#E7600) following the manufacturer’s instructions. The libraries were then sequenced using paired end sequencing with an Illumina NovaSeq 6000.

Bioinformatic analysis

The adapter and low-quality sequences were removed using the fastp software with default parameters67. The quality-filtered reads were mapped to both the P. japonicum68 and Arabidopsis genome (TAIR10) using STAR69 and were separated based on mapping to P. japonicum and Arabidopsis reads. The separated reads were then re-mapped to their respective genomes. The read count was calculated using FeatureCounts70. The differential expression analysis was used to identify differentially expressed (DE) genes between treatments and time points and was performed using Deseq2 with the default settings and q-value < 0.0571 (Supplementary Data 28). The gene expression clustering was performed using the Mfuzz software72. Custom annotations of the P. japonicum predicted proteins68 were estimated using InterProScan73, these were used for Gene ontology analysis that was performed using the topGO software74. ABA and cytokinin responsive genes in P. japonicum (Supplementary Data 9) were identified using the tBLASTp and tBLASTp algorithm of the Arabidopsis ABA and cytokinin responsive genes described by75 or Arabidopsis genes responsive to SA described in76 against the P. japonicum genome68. Cell cycle and ROS related genes (Supplementary Data 9) were identified using the tBLASTp and tBLASTn algorithm of the Arabidopsis cell cycle and ROS related genes described77,78 in against the P. japonicum genome68.


Statistical analyses were performed using one-way ANOVA followed by Tukey’s HSD post-hoc test. The results of this statistical analysis are represented by compact letter display; treatments with different letters are significantly different with p-value<0.05 whereas treatments with the same letter/letters are not significantly different. For haustoria per P. japonicum and xylem bridge formation percentage data, the statistical analyses were performed on the means of at least 2 biological replicates, where each biological replicate consisted of 20 plants. For single comparisons, two tailed student’s t-tests was used.


P. japonicum seedlings were grown for five days before transferring to nutrient-free 0.8% (w/v) agar medium or 0.8% (w/v) agar medium supplemented with ½MS, ½MS no N or 5 μM ABA for 5 days. Additionally, P. japonicum seedlings were placed on pots containing 100:0, 50:50, 33:66, 25:75 soil:sand ratios. The pots were placed at 25oC and long-day conditions (16 h light:8 h dark and 100 μmol m−2 s−1) and 60% humidity for 1.5 months. During this time the plants were provided deionized water. The seedlings or the shoots and roots of the above described P. japonicum were then harvested and RNA extraction was performed using the ROTI®Prep RNA MINI (Roth) kit following the manufacturer’s instructions. The extracted RNA was then treated with DNase I (Thermo Scientific™) following the manufacturer’s instructions. cDNA synthesis was performed using Maxima First Strand cDNA Synthesis Kit for RT-qPCR (Thermo Scientific™) following the manufacturer’s instructions. PjPTB14 was used as an internal control. qPCR was performed with SYBR-Green master mix (Applied Biosystems™). The relative expression was calculated using the Pfaffl method79. All experiments were repeated at least three times with at least two technical replications each. For statistical analysis, the student’s t-test was used. The primers used for this experiment are listed in Supplementary Data 10. 4 plants per sample were collected and these experiments were replicated three times.

Hormonal quantifications

P. japonicum seedlings were grown for four to five days before transferring to nutrient-free 0.8% (w/v) agar medium or 0.8% (w/v) agar medium supplemented with 10.3 mM NH4NO3 for three days. Arabidopsis Col-0 or aba2-1 was placed next to the P. japonicum seedlings and left for 10 days. P. japonicum seedlings without a host were used as control. After 10 days with or without the presence of a host, four entire P. japonicum seedlings per sample and four to five entire Arabidopsis seedlings per sample were collected. For the mature P. japonicum root measurements, ~1-month-old P. japonicum was transferred to nutrient-free 0.8% (w/v) agar medium or 0.8% (w/v) agar medium supplemented with 10.3 mM NH4NO3 for seven days before Arabidopsis Col-0 addition. 4 roots per sample were collected at 10 dpi. The samples were crushed to powder using liquid N with mortar and pestle. Samples were extracted, purified and analyzed according to a previously published method80. Approximately 20 mg of frozen material per sample was homogenized and extracted in 1 mL of ice-cold 50% aqueous acetonitrile (v/v) with the mixture of 13C- or deuterium-labeled internal standards using a bead mill (27 hz, 10 min, 4 °C; MixerMill, Retsch GmbH, Haan, Germany) and sonicator (3 min, 4 °C; Ultrasonic bath P 310 H, Elma, Germany). After centrifugation (20000 × g, 15 min, 4 °C), the supernatant was purified as following. A solid-phase extraction column Oasis HLB (30 mg 1 cc, Waters Inc., Milford, MA, USA) was conditioned with 1 ml of 100% methanol and 1 ml of deionized water (Milli-Q, Merck Millipore, Burlington, MA, USA). After the conditioning steps each sample was loaded on SPE column and flow-through fraction was collected together with the elution fraction 1 ml 30% aqueous acetonitrile (v/v). Samples were evaporated to dryness using speed vac (SpeedVac SPD111V, Thermo Scientific, Waltham, MA, USA). Prior LC-MS analysis, samples were dissolved in 40 µL of 30% acetonitrile (v/v) and transferred to insert-equipped vials. Mass spectrometry analysis of targeted compounds was performed by an UHPLC-ESI-MS/MS system comprising of a 1290 Infinity Binary LC System coupled to a 6490 Triple Quad LC/MS System with Jet Stream and Dual Ion Funnel technologies (Agilent Technologies, Santa Clara, CA, USA). The quantification was carried out in Agilent MassHunter Workstation Software Quantitative (Agilent Technologies, Santa Clara, CA, USA). These experiments were repeated 4 times.

Plasmid construction and P. japonicum transformation

Plasmid construction was done using modules of Greengate cloning81 (Addgene). For the entry modules, the pMAS promoter, terMAS terminator, and DsRed reporter cassette were amplified from pAGM4723 using primers with the addition of BsaI restriction sites and respective overhangs on the 5’ends (Supplementary Data 10), then inserted into Greengate modules pGGA000, pGGE000, and pGGF000, to create pGGA-pMAS, pGGE-terMAS, and pGGF-DsRed modules, respectively. The CDS of Atabi1-1 was amplified from the cDNA of Arabidopsis abi1-1 mutant, then inserted into pGGC000 to create pGGC-abi1. All of the restriction and ligation reactions were done using BsaI-HF and T4 ligase (NEB), respectively. The resulted plasmids were transformed into E. coli using chemically competent cells (Subcloning Efficiency™ DH5α Competent Cells, ThermoFisher Scientific) according to the manufacturer’s protocol. The transformed cells were cultured and selected on LB medium with 100 μg/mL ampicillin. The plasmids were extracted using Plasmid DNA Miniprep Kit (ThermoFisher), and the sequences were confirmed by sequencing of the ligation sites (Macrogen).

To create the final binary vector pGG-abi1, the Greengate reaction was performed using the previously described protocol81 using the entry vectors pGGA-pMAS, pGGB003, pGGC-abi1, pGGD002, pGGE-terMAS, pGGF-DsRed, and the empty destination vector pGGZ001. The reaction product was used for E. coli transformation, then the cells were cultured on LB medium with 100 μg/mL spectinomycin. The sequence was initially confirmed by digestion analysis, then sequencing of the ligation site. The plasmid was then inserted in electrocompetent Agrobacterium rhizogenes strain AR1193 then the cells were cultured on LB medium with 100 μg/mL spectinomycin and 50 μg/mL rifampicin.

P. japonicum transformation was performed according to a previously published method36. Briefly, three to four-day-old P. japonicum seedlings were sonicated for 10 to 15 seconds followed by vacuum infiltration for 5 minutes with suspension of Agrobacterium rhizogenes strain AR1193 carrying the overexpressing pMAS::Atabi1-1 construct. The seedlings were then transferred on co-cultivation media (Gamborg’s B5 medium, 0.8% agar, 1% sucrose, 450 μM acetosyringone) at 22 °C for 2 days in the dark conditions. Later, plants were transferred on Gamborg’s B5 medium supplemented with antibiotic (0.8% agar, 1% sucrose, 300 μg/ml cefotaxime) and incubated at 25 °C under long-day conditions for ~1 month. Hairy roots expressing the construct were identified by red fluorescence using a Leica M205 FA fluorescence stereo microscope. Roots were selected based on their florescent status before being placed on nutrient-free 0.8% (w/v) agar medium or 0.8% (w/v) agar medium supplemented by ½MS or ½MS no N for 3 days prior to Arabidopsis (Col-0) host application. Haustoria numbers were estimated at 7 dpi. This experiment was replicated three times. Construct expression levels were estimated by qPCR using Atabi1-1 primers (Supplementary Data 10).

Striga-rice Infection in the rhizotron system

The rice infection was performed in a rhizotron system63. 7-day-old rice seedlings were transferred to the rhizotron (10-cm × 14-cm-square petri dish with top and bottom perforation for shoot growth and water draining, filled with same size of rockwool [Nichiasu, Tokyo, Japan] onto which a 100 μm nylon mesh was placed) and fertilized with 25 mL half-strength Murashige & Skoog media per rhizotron. The root parts of the rhizotron were covered with aluminum foil and placed vertically in a growth chamber at 12-h light: 28 oC /12-h dark: 20 oC cycles for 2 weeks before S. hermonthica infection. Rice seedlings were inoculated with S. hermonthica seeds by placing Strigol-treated S. hermonthica carefully along rice roots with 5 mm intervals. Each rhizotron was inoculated by 20-60 S. hermonthica seeds. The rhizotron containing inoculated rice seedlings were incubated in the growth chamber described above, and developmental stages of S. hermonthica were categorized with a stereomicroscope (Zeiss Stemi 2000-C) after 2 and 4 weeks. Successful infection rates were calculated by the number of S. hermonthica with more than three leaf pairs divided by the total infected S. hermonthica seeds. Each rhizotron was watered with 25 mL of indicated nutrient or chemical containing solutions two times per week. The chemical concentrations used in this study were as following; 10.3 mM ammonium nitrate, 1.09 mM monosodium phosphate, 20.6 mM potassium nitrate, 0.62 mM monopotassium phosphate, 10 µM gibberellic acid, 0.08 nM 6-benzylaminopurine, 10 µM paclobutrazol, 10 or 100 µM fluridone, and 10 or 100 µM abscisic acid, 10.3 mM NH4Cl, 19.69 mM KNO3, 500 nM IAA or 500 nM NAA. 8 plants per sample were used and these experiments we replicated at least 3 times.

Reporting summary

Further information on research design is available in the Nature Research Reporting Summary linked to this article.

Data availability

Sequence data are available at the Gene Expression Omnibus under accession numbers GSE177484. Sequence data of the Phtheirospermum japonicum genes studied in this article are available in GenBank ( under the accession numbers provided in Supplementary Data 11. Other experimental data shown in this study are provided in the Source Data file.


  1. De Groote, H., Wangare, L. & Kanampiu, F. Evaluating the use of herbicide-coated imidazolinone-resistant (IR) maize seeds to control Striga in farmers’ fields in Kenya. Crop Prot. 26, 1496–1506 (2007).

    Article  CAS  Google Scholar 

  2. Heide-Jørgensen, H. S. Parasitic Flowering Plants 438 (Brill, 2008).

  3. Rodenburg, J., Demont, M., Zwart, S. J. & Bastiaans, L. Parasitic weed incidence and related economic losses in rice in Africa. Agric. Ecosyst. Environ. 235, 306–317 (2016).

    Article  Google Scholar 

  4. Spallek, T., Mutuku, M. & Shirasu, K. The genus Striga: a witch profile. Mol. Plant Pathol. 14, 861–869 (2013).

    PubMed  PubMed Central  Article  Google Scholar 

  5. Kuijt, J. & Others. The Biology of Parasitic Flowering Plants (University of California Press,1969).

  6. Barkman, T. J. et al. Mitochondrial DNA suggests at least 11 origins of parasitism in angiosperms and reveals genomic chimerism in parasitic plants. BMC Evol. Biol. 7, 248 (2007).

    PubMed  PubMed Central  Article  CAS  Google Scholar 

  7. Kokla, A. & Melnyk, C. W. Developing a thief: Haustoria formation in parasitic plants. Dev. Biol. 442, 53–59 (2018).

    CAS  PubMed  Article  Google Scholar 

  8. Spallek, T. et al. Interspecies hormonal control of host root morphology by parasitic plants. Proc. Natl Acad. Sci. USA 114, 5283–5288 (2017).

    CAS  PubMed  PubMed Central  Article  Google Scholar 

  9. Shahid, S. et al. MicroRNAs from the parasitic plant Cuscuta campestris target host messenger RNAs. Nature 553, 82–85 (2018).

    ADS  CAS  PubMed  Article  Google Scholar 

  10. Liu, N. et al. Extensive inter-plant protein transfer between Cuscuta parasites and their host plants. Mol. Plant (2020).

  11. Chang, M. & Lynn, D. G. The haustorium and the chemistry of host recognition in parasitic angiosperms. J. Chem. Ecol. 12, 561–579 (1986).

    CAS  PubMed  Article  Google Scholar 

  12. Wada, S., Cui, S. & Yoshida, S. Reactive oxygen species (ROS) generation is indispensable for haustorium formation of the root parasitic plant Striga hermonthica. Front. Plant Sci. 10, 328 (2019).

    PubMed  PubMed Central  Article  Google Scholar 

  13. Cui, S. et al. Haustorial hairs are specialized root hairs that support parasitism in the facultative parasitic plant Phtheirospermum japonicum. Plant Physiol. 170, 1492–1503 (2016).

    CAS  PubMed  Article  Google Scholar 

  14. Ishida, J. K. et al. Local auxin biosynthesis mediated by a YUCCA flavin monooxygenase regulates haustorium development in the parasitic plant Phtheirospermum japonicum. Plant Cell 28, 1795–1814 (2016).

    CAS  PubMed  PubMed Central  Article  Google Scholar 

  15. Wakatake, T., Yoshida, S. & Shirasu, K. Induced cell fate transitions at multiple cell layers configure haustorium development in parasitic plants. Development 145, dev164848 (2018).

  16. Heide-Jorgensen & Kuijt, J. The haustorium of the root parasite triphysaria (scrophulariaceae), with special reference to xylem bridge ultrastructure. Am. J. Bot. 82, 782–797 (1995).

    Article  Google Scholar 

  17. Mwangangi, I. M., Haefele, S. M., Bastiaans, L., Runo, S. & Rodenburg, J. Combining host plant defence with targeted nutrition: key to durable control of hemi-parasitic Striga in cereals in sub-Saharan Africa. New Phytol. 230, 2164–2178 (2021).

  18. Jamil, M., Kanampiu, F. K., Karaya, H., Charnikhova, T. & Bouwmeester, H. J. Striga hermonthica parasitism in maize in response to N and P fertilisers. Field Crops Res. 134, 1–10 (2012).

    Article  Google Scholar 

  19. Yoneyama, K. et al. Nitrogen deficiency as well as phosphorus deficiency in sorghum promotes the production and exudation of 5-deoxystrigol, the host recognition signal for arbuscular mycorrhizal fungi and root parasites. Planta 227, 125–132 (2007).

    CAS  PubMed  Article  Google Scholar 

  20. Yoneyama, K., Yoneyama, K., Takeuchi, Y. & Sekimoto, H. Phosphorus deficiency in red clover promotes exudation of orobanchol, the signal for mycorrhizal symbionts and germination stimulant for root parasites. Planta 225, 1031–1038 (2007).

    CAS  PubMed  Article  Google Scholar 

  21. Sun, H. et al. Strigolactones are involved in phosphate- and nitrate-deficiency-induced root development and auxin transport in rice. J. Exp. Bot. 65, 6735–6746 (2014).

    CAS  PubMed  PubMed Central  Article  Google Scholar 

  22. Igbinnosa, I., Cardwell, K. F. & Okonkwo, S. N. C. The effect of nitrogen on the growth and development of giant witchweed,Striga hermonthica Benth.: effect on cultured germinated seedlings in host absence. Eur. J. Plant Pathol. 102, 77–86 (1996).

    Article  Google Scholar 

  23. Davies, D. M. & Graves, J. D. The impact of phosphoras on interactions of the hemiparasitic angiosperm Rhinanthus minor and its host Lolium perenne. Oecologia 124, 100–106 (2000).

    ADS  CAS  PubMed  Article  Google Scholar 

  24. Zhang, H. & Forde, B. G. Regulation of Arabidopsis root development by nitrate availability. J. Exp. Bot. 51, 51–59 (2000).

    CAS  PubMed  Article  Google Scholar 

  25. Alboresi, A. et al. Nitrate, a signal relieving seed dormancy in Arabidopsis. Plant Cell Environ. 28, 500–512 (2005).

    CAS  PubMed  Article  Google Scholar 

  26. Castro Marín, I. et al. Nitrate regulates floral induction in Arabidopsis, acting independently of light, gibberellin and autonomous pathways. Planta 233, 539–552 (2011).

    PubMed  Article  CAS  Google Scholar 

  27. Samuelson, M. E. & Larsson, C.-M. Nitrate regulation of zeatin riboside levels in barley roots: effects of inhibitors of N assimilation and comparison with ammonium Mariann. Plant Sci. 93, 77–84 (1994).

    Article  Google Scholar 

  28. Takei, K., Sakakibara, H., Taniguchi, M. & Sugiyama, T. Nitrogen-dependent accumulation of cytokinins in root and the translocation to leaf: Implication of cytokinin species that induces gene expression of maize response regulator. Plant Cell Physiol. 42, 85–93 (2001).

    CAS  PubMed  Article  Google Scholar 

  29. Takei, K. et al. AtIPT3 is a key determinant of nitrate-dependent cytokinin biosynthesis in Arabidopsis. Plant Cell Physiol. 45, 1053–1062 (2004).

    CAS  PubMed  Article  Google Scholar 

  30. Kamada-Nobusada, T., Makita, N., Kojima, M. & Sakakibara, H. Nitrogen-dependent regulation of de novo cytokinin biosynthesis in rice: the role of glutamine metabolism as an additional signal. Plant Cell Physiol. (2013).

    Article  PubMed  PubMed Central  Google Scholar 

  31. Landrein, B. et al. Nitrate modulates stem cell dynamics in Arabidopsis shoot meristems through cytokinins. Proc. Natl Acad. Sci. 115, 1382–1387 (2018).

    CAS  PubMed  PubMed Central  Article  Google Scholar 

  32. Vidal, E. A. et al. Nitrate-responsive miR393/AFB3 regulatory module controls root system architecture in Arabidopsis thaliana. Proc. Natl Acad. Sci. USA 107, 4477–4482 (2010).

    ADS  CAS  PubMed  PubMed Central  Article  Google Scholar 

  33. Ondzighi-Assoume, C. A., Chakraborty, S. & Harris, J. M. Environmental nitrate stimulates abscisic acid accumulation in arabidopsis root tips by releasing it from inactive stores. Plant Cell 28, 729–745 (2016).

    CAS  PubMed  PubMed Central  Article  Google Scholar 

  34. Signora, L., De Smet, I., Foyer, C. H. & Zhang, H. ABA plays a central role in mediating the regulatory effects of nitrate on root branching in Arabidopsis. Plant J. 28, 655–662 (2001).

    CAS  PubMed  Article  Google Scholar 

  35. Oswald, A. Striga control—technologies and their dissemination. Crop Prot. 24, 333–342 (2005).

    Article  Google Scholar 

  36. Ishida, J. K., Yoshida, S., Ito, M., Namba, S. & Shirasu, K. Agrobacterium rhizogenes-mediated transformation of the parasitic plant Phtheirospermum japonicum. PLoS ONE 6, e25802 (2011).

    ADS  CAS  PubMed  PubMed Central  Article  Google Scholar 

  37. Wakatake, T., Ogawa, S. Yoshida, S. & Shirasu, K. An auxin transport network underlies xylem bridge formation between the hemi-parasitic plant Phtheirospermum japonicum and host Arabidopsis. Development 147, dev187781 (2019).

  38. Laohavisit, A. et al. Quinone perception in plants via leucine-rich-repeat receptor-like kinases. Nature 587, 92–97 (2020).

  39. Verslues, P. E. & Bray, E. A. Role of abscisic acid (ABA) and Arabidopsis thaliana ABA-insensitive loci in low water potential-induced ABA and proline accumulation. J. Exp. Bot. 57, 201–212 (2006).

    CAS  PubMed  Article  Google Scholar 

  40. Leung, J. et al. The role of ABI1 in abscisic acid signal transduction: from gene to cell. Symp. Soc. Exp. Biol. 51, 65–71 (1998).

    CAS  PubMed  Google Scholar 

  41. Ramachandran, P. et al. Abscisic acid signaling activates distinct VND transcription factors to promote xylem differentiation in Arabidopsis. Curr. Biol. (2021).

  42. Cechin, I. & Press, M. C. Nitrogen relations of the sorghum‐Striga hermonthica host‐parasite association: germination, attachment and early growth. N. Phytol. 124, 681–687 (1993).

    CAS  Article  Google Scholar 

  43. Fujioka, H. et al. Aberrant protein phosphatase 2C leads to abscisic acid insensitivity and high transpiration in parasitic Striga. Nat. Plants 5, 258–262 (2019).

  44. Irving, L. J. et al. Host nutrient supply affects the interaction between the hemiparasite Phtheirospermum japonicum and its host Medicago sativa. Environ. Exp. Bot. 162, 125–132 (2019).

    CAS  Article  Google Scholar 

  45. Bouguyon, E. et al. Multiple mechanisms of nitrate sensing by Arabidopsis nitrate transceptor NRT1.1. Nat. Plants 1, 15015 (2015).

    CAS  PubMed  Article  Google Scholar 

  46. Araya, T., Kubo, T., von Wirén, N. & Takahashi, H. Statistical modeling of nitrogen-dependent modulation of root system architecture in Arabidopsis thaliana. J. Integr. Plant Biol. 58, 254–265 (2016).

    CAS  PubMed  Article  Google Scholar 

  47. Zhang, H., Jennings, A., Barlow, P. W. & Forde, B. G. Dual pathways for regulation of root branching by nitrate. Proc. Natl Acad. Sci. USA 96, 6529–6534 (1999).

    ADS  CAS  PubMed  PubMed Central  Article  Google Scholar 

  48. Schultze, M. & Kondorosi, A. Regulation of symbiotic root nodule development. Annu. Rev. Genet. 32, 33–57 (1998).

    CAS  PubMed  Article  Google Scholar 

  49. Carroll, B. J., McNeil, D. L. & Gresshoff, P. M. A supernodulation and nitrate-tolerant symbiotic (nts) soybean mutant. Plant Physiol. 78, 34–40 (1985).

    CAS  PubMed  PubMed Central  Article  Google Scholar 

  50. Caba, J. M., Recalde, L. & Ligero, F. Nitrate-induced ethylene biosynthesis and the control of nodulation in alfalfa. Plant Cell Environ. 21, 87–93 (1998).

    CAS  Article  Google Scholar 

  51. Reid, D. E., Ferguson, B. J., Hayashi, S., Lin, Y.-H. & Gresshoff, P. M. Molecular mechanisms controlling legume autoregulation of nodulation. Ann. Bot. 108, 789–795 (2011).

    CAS  PubMed  PubMed Central  Article  Google Scholar 

  52. Gautrat, P. et al. Unraveling new molecular players involved in the autoregulation of nodulation in Medicago truncatula. J. Exp. Bot. 70, 1407–1417 (2019).

    CAS  PubMed  PubMed Central  Article  Google Scholar 

  53. Lin, J., Roswanjaya, Y. P., Kohlen, W., Stougaard, J. & Reid, D. Nitrate inhibits nodule organogenesis through inhibition of cytokinin biosynthesis in Lotus japonicus. bioRxiv (2020).

  54. Sasaki, T. et al. Shoot-derived cytokinins systemically regulate root nodulation. Nat. Commun. 5, 4983 (2014).

    ADS  CAS  PubMed  Article  Google Scholar 

  55. Jiang, F., Jeschke, W. D. & Hartung, W. Abscisic acid (ABA) flows from Hordeum vulgare to the hemiparasite Rhinanthus minor and the influence of infection on host and parasite abscisic acid relations. J. Exp. Bot. 55, 2323–2329 (2004).

    CAS  PubMed  Article  Google Scholar 

  56. Furuhashi, T. et al. Morphological and plant hormonal changes during parasitization by Cuscuta japonica on Momordica charantia. J. Plant Interact. 9, 220–232 (2014).

    CAS  Article  Google Scholar 

  57. Taylor, A., Martin, J. & Seel, W. E. Physiology of the parasitic association between maize and witchweed (Striga hermonthica): is ABA involved? J. Exp. Bot. 47, 1057–1065 (1996).

    CAS  Article  Google Scholar 

  58. Frost et al. J. D. Striga hermonthica reduces photosynthesis in sorghum: the importance of stomatal limitations and a potential role for ABA? Plant Cell Environ. 20, 483–492 (1997).

    CAS  Article  Google Scholar 

  59. Li, J. et al. The parasitic plant cuscuta australis is highly insensitive to abscisic acid-induced suppression of hypocotyl elongation and seed germination. PLoS ONE 10, e0135197 (2015).

  60. Ding, Y. et al. Abscisic acid coordinates nod factor and cytokinin signaling during the regulation of nodulation in Medicago truncatula. Plant Cell 20, 2681–2695 (2008).

    CAS  PubMed  PubMed Central  Article  Google Scholar 

  61. Suzuki, A. et al. Control of nodule number by the phytohormone abscisic acid in the roots of two leguminous species. 45, 914–922 (2004).

  62. Tominaga, A. et al. Effect of abscisic acid on symbiotic nitrogen fixation activity in the root nodules of Lotus japonicus. Plant Signal. Behav. 5, 440–443 (2010).

    CAS  PubMed  PubMed Central  Article  Google Scholar 

  63. Yoshida, S. & Shirasu, K. Multiple layers of incompatibility to the parasitic witchweed, Striga hermonthica. N. Phytol. 183, 180–189 (2009).

    Article  Google Scholar 

  64. González-Guzmán, M. et al. The short-chain alcohol dehydrogenase ABA2 catalyzes the conversion of xanthoxin to abscisic aldehyde. Plant Cell 14, 1833–1846 (2002).

    PubMed  PubMed Central  Article  CAS  Google Scholar 

  65. Umezawa, T. et al. Type 2C protein phosphatases directly regulate abscisic acid-activated protein kinases in Arabidopsis. Proc. Natl Acad. Sci. USA 106, 17588–17593 (2009).

    ADS  CAS  PubMed  PubMed Central  Article  Google Scholar 

  66. Hirayama, K. & Mori, K. Synthesis of (+)-strigol and (+)-orobanchol, the germination stimulants, and their stereoisomers by employing lipase-catalyzed asymmetric acetylationas the key step. Eur. J. Org. Chem. 1999, 2211–2217 (1999).

    Article  Google Scholar 

  67. Chen, S., Zhou, Y., Chen, Y. & Gu, J. fastp: an ultra-fast all-in-one FASTQ preprocessor. Bioinformatics 34, i884–i890 (2018).

    PubMed  PubMed Central  Article  CAS  Google Scholar 

  68. Cui, S. et al. Ethylene signaling mediates host invasion by parasitic plants. Sci. Adv. 6, eabc2385 (2020).

  69. Dobin, A. et al. STAR: ultrafast universal RNA-seq aligner. Bioinformatics 29, 15–21 (2013).

  70. Liao, Y., Smyth, G. K. & Shi, W. featureCounts: an efficient general purpose program for assigning sequence reads to genomic features. Bioinformatics 30, 923–930 (2014).

    CAS  PubMed  Article  Google Scholar 

  71. Love, M., Anders, S. & Huber, W. Differential analysis of count data–the DESeq2 package. Genome Biol. 15, 550 (2014).

    PubMed  PubMed Central  Article  CAS  Google Scholar 

  72. Kumar, L. & Futschik, M. E. Mfuzz: a software package for soft clustering of microarray data. Bioinformation 2, 5–7 (2007).

  73. Blum, M. et al. The InterPro protein families and domains database: 20 years on. Nucleic Acids Res. 49, D344–D354 (2020).

    PubMed Central  Article  CAS  Google Scholar 

  74. Alexa, A. & Rahnenfuhrer, J. topGO: Enrichment Analysis for Gene Ontology. R package version 2.48.0. (2022).

  75. Nemhauser, J. L., Hong, F. & Chory, J. Different plant hormones regulate similar processes through largely nonoverlapping transcriptional responses. Cell 126, 467–475 (2006).

    CAS  PubMed  Article  Google Scholar 

  76. Blanco, F. et al. Identification of NPR1-dependent and independent genes early induced by salicylic acid treatment in arabidopsis. Plant Mol. Biol. 59, 927–944 (2005).

    CAS  PubMed  Article  Google Scholar 

  77. Oliveira, R. A. et al. Analysis of Arabidopsis thaliana redox gene network indicates evolutionary expansion of class III peroxidase in plants. Sci. Rep. 9, 15741 (2019).

    ADS  PubMed  PubMed Central  Article  CAS  Google Scholar 

  78. Vandepoele, K. et al. Genome-wide analysis of core cell cycle genes in Arabidopsis. Plant Cell 14, 903–916 (2002).

    CAS  PubMed  PubMed Central  Article  Google Scholar 

  79. Pfaffl, M. W. A new mathematical model for relative quantification in real-time RT-PCR. Nucleic Acids Res. 29, e45 (2001).

    CAS  PubMed  PubMed Central  Article  Google Scholar 

  80. Šimura, J. et al. Plant hormonomics: Multiple phytohormone profiling by targeted metabolomics. Plant Physiol. 177, 476–489 (2018).

    PubMed  PubMed Central  Article  CAS  Google Scholar 

  81. Lampropoulos, A. et al. GreenGate—a novel, versatile, and efficient cloning system for plant transgenesis. PLoS ONE 8, e83043 (2013).

    ADS  PubMed  PubMed Central  Article  CAS  Google Scholar 

Download references


The authors thank Annelie Carlsbecker and Prashanth Ramachandran for providing abi1-1C seeds, and Thomas Spallek for critical reading of the manuscript. A.K., M.L., T.S. and C.W.M. were supported by a Wallenberg Academy Fellowship (2016-0274) and an ERC starting grant (GRASP- 805094). K.L. and J.S. were supported by grants from the Swedish Research Council, the Swedish Governmental Agency for Innovation Systems and the Knut and Alice Wallenberg Foundation. S.Y., S.C., and X.Z. were supported by MEXT KAKENHI (JP20H05909), and S.C. by KAKENHI no. 19K16169. The authors acknowledge support from the Uppsala Multidisciplinary Center for Advanced Computational Science for assistance with access to the UPPMAX computational infrastructure. We also thank the Swedish Metabolomics Centre for access to instrumentation.


Open access funding provided by Swedish University of Agricultural Sciences.

Author information

Authors and Affiliations



A.K. and C.W.M. conceived the experiments. A.K., M.L., X.Z., T.S., and J.S. performed the experiments. S.C., S.Y., K.L., and C.W.M. supervised the experiments. A.K. and C.W.M. wrote the paper. All authors edited and revised the final paper.

Corresponding author

Correspondence to Charles W. Melnyk.

Ethics declarations

Competing interests

The authors declare no competing interests.

Peer review

Peer review information

Nature Communications thanks Jianqiang Wu and the other, anonymous, reviewer(s) for their contribution to the peer review of this work. Peer reviewer reports are available.

Additional information

Publisher’s note Springer Nature remains neutral with regard to jurisdictional claims in published maps and institutional affiliations.

Supplementary information

Source data

Rights and permissions

Open Access This article is licensed under a Creative Commons Attribution 4.0 International License, which permits use, sharing, adaptation, distribution and reproduction in any medium or format, as long as you give appropriate credit to the original author(s) and the source, provide a link to the Creative Commons license, and indicate if changes were made. The images or other third party material in this article are included in the article’s Creative Commons license, unless indicated otherwise in a credit line to the material. If material is not included in the article’s Creative Commons license and your intended use is not permitted by statutory regulation or exceeds the permitted use, you will need to obtain permission directly from the copyright holder. To view a copy of this license, visit

Reprints and Permissions

About this article

Verify currency and authenticity via CrossMark

Cite this article

Kokla, A., Leso, M., Zhang, X. et al. Nitrogen represses haustoria formation through abscisic acid in the parasitic plant Phtheirospermum japonicum. Nat Commun 13, 2976 (2022).

Download citation

  • Received:

  • Accepted:

  • Published:

  • DOI:


By submitting a comment you agree to abide by our Terms and Community Guidelines. If you find something abusive or that does not comply with our terms or guidelines please flag it as inappropriate.


Quick links

Nature Briefing

Sign up for the Nature Briefing newsletter — what matters in science, free to your inbox daily.

Get the most important science stories of the day, free in your inbox. Sign up for Nature Briefing