The sampling of Meconopsis petals was approved by the Administration Bureau of Sichuan Wolong National Nature Reserve. Petals of M. balangensis, M. punicea, and M. integrifolia were used as experimental materials. Samples were selected at five flowering stages (S1–S5) (Figure 1A) in June 2023 from approximately 4,000 m elevation in the Balang Mountain, Xiaojin County, Sichuan Province, China (102°53′E, 30°55′N). The five developmental stages included the early bud (S1), late bud (S2), early flowering (S3), full bloom (S4), and late flowering (S5) stages. A portion of the fresh petals was used to measure color parameters (L*, a*, b*, C*) and for scanning electron microscopy (SEM) observation. Remaining samples were immediately frozen in liquid nitrogen and stored at −80 °C.

Petals of M. argemonantha at full bloom (Figure 1B) were collected from approximately 4,200 m elevation on Zhari Mountain, Longzi County, Shannan City, Tibet Autonomous Region, China (92°58′E, 28°40′N) Samples were immediately frozen in liquid nitrogen after collection, transported to the laboratory, and stored at −80 °C. The four species were abbreviated as Mb, Mp, Mi, and Ma, respectively.

Color phenotypes of Meconopsis tepals at three developmental stages were measured using a colorimeter (CM-2600d, Konica Minolta, Japan). Lightness (L*) and hue values (a* and b*) were recorded for each petal sample. L*, a*, and b* represent the three coordinates in the CIE Lab color space, collectively describing color appearance. L* represents brightness ranging from black (0) to white (100); a* ranges from red (positive) to green (negative); b* ranges from yellow (positive) to blue (negative). Chroma (C*) was calculated using the formula C* = (a² + b²)¹^/², representing color saturation (Gonnet, 2001). Five petals from each plant were measured three times. The mean of five plants was used as the representative color value for each species.

Petals at full bloom were cut into 5 mm × 5 mm squares and immediately immersed in 3% glutaraldehyde fixative. Fixed samples were washed three times with ultrapure water (UP) for 10 min each. After post-fixation with 1% osmium tetroxide for 1 h, the samples were again washed three times with UP water for 10 min each. Samples were dehydrated through a graded ethanol series (30%, 50%, 70%, 80%, 90%, 95%, 100%), with each step lasting 15 min. Samples were dried using a critical-point dryer, mounted on stubs with conductive adhesive and sputter-coated using an ion coater. Finally, the samples were examined and imaged using a scanning electron microscope (SEM) (He et al., 2021).

Chlorophyll and carotenoid contents in Meconopsis tepals were quantified using a plant chlorophyll content detection kit (Jiancheng, Nanjing, China) according to the manufacturer’s protocol. Fresh petals were ground into fine powder under liquid nitrogen, and 0.05 g of the powder was used. Anhydrous ethanol and acetone were mixed at a 1:2 (v/v) ratio to prepare the extraction solution. To the prepared sample, 0.5 mL distilled water and 50 mg of Reagent 1 were added and mixed thoroughly. The total volume was adjusted to 2.5 mL, and samples were extracted in the dark for approximately 3 h until the residue turned white, indicating complete extraction. The mixture was centrifuged at 4,000 rpm for 10 min. Using the extraction solution as a blank, absorbance values were measured at 470, 663, and 645 nm, denoted as A₄₇₀, A₆₆₃, and A₆₄₅, respectively. Three biological replicates were conducted for each sample. Chlorophyll and carotenoid contents were calculated as follows:

Where Ca refers to chlorophyll a content, C_b refers to chlorophyll b content, C_T refers to total chlorophyll content, and Car refers to carotenoid content. V is the total volume of the extract (2.5 mL), F is the dilution factor (1), and W is the weight of the sample (0.05 g).

Flavonoid content was measured using a colorimetric flavonoid assay kit (Jiancheng, Nanjing, China) according to the manufacturer’s protocol. Petal samples were ground in liquid nitrogen, and ~0.05 g of powder was placed into a centrifuge tube. Subsequently, 2 mL of 60% ethanol was added, and samples were extracted with shaking at 60 °C for 2 h. After extraction, samples were centrifuged at 10,000 rpm for 10 min at 25 °C, and the supernatant was collected as the flavonoid extract. Subsequent procedures followed the manufacturer’s instructions. Three biological replicates were set up for each sample.

The total anthocyanin content in petals was determined using the Enzyme-linked Biological Total Anthocyanin Extraction Kit (Meilian, Shanghai, China), following the manufacturer’s instructions. A 0.1 g petal sample was mixed with 1 mL extraction solution, homogenized thoroughly, and transferred to an EP tube. The volume of the extraction solution was adjusted to 1 mL. The tube was tightly capped and subjected to extraction at 60 °C for 30 min with several shaking intervals. The sample was centrifuged at 12,000 rpm for 10 min at 25 °C, and the supernatant was collected. Subsequent operations were performed according to the kit instructions. Three biological replicates were set up for each sample.

Petals of three color variants at three developmental stages (S1, S3, S4; Figure 1A) were frozen in liquid nitrogen and ground into powder. Then, 0.02 g of powdered petals was placed in a 1.5 mL tube, homogenized with 0.1 mL distilled water, and centrifuged at 12,000 rpm for 15 min at 4 °C. The pH of the supernatant was measured three times at 25 °C using a pH meter (Yuan et al., 2024). Five biological replicates were analyzed per species, each with four technical replicates.

The petals at the full-bloom stage of the four flower colors were used as the experimental materials (Figure 1B), and they were crushed with a mixing grinder equipped with zirconia beads. A 0.1 g aliquot of the powdered sample was extracted. After centrifugation at 12,000 rpm for 10 min, the extract was filtered and analyzed using ultra-high-performance liquid chromatography (UPLC). All chromatographic separations were performed using an UltiMate 3000 UPLC system (Thermo Fisher Scientific, Bremen, Germany). A high-resolution Q Exactive™ hybrid quadrupole-Orbitrap mass spectrometer (Thermo Fisher Scientific) was used to detect metabolites eluted from the column. Quality control (QC) samples were prepared by mixing equal volumes of petal extracts from white, blue, red, and yellow Meconopsis morphotypes. Four biological replicates were included in this assay. Variable importance in projection (VIP) values, P-values, and fold changes (FC) were used to identify differentially accumulated metabolites (DAMs). Metabolites were considered significant with VIP ≥ 1, P< 0.05, and FC ≥ 2 or ≤ 0.5.

The same batch of full-bloom petals from four color varieties used for UPLC–MS/MS detection was submitted to Hangzhou Lianchuan Biotechnology (China) for RNA sequencing, with three biological replicates. Total RNA was extracted from petal samples using the RNAprep Pure Plant Kit (DP441, Tiangen, China) according to the manufacturer’s protocol and assessed for integrity, purity and concentration. cDNA libraries were sequenced on the Illumina NovaSeq™ 6000 platform to obtain raw reads. Quality control was applied to remove adapters, primers, and low-quality reads, generating high-quality clean data. Clean reads were de novo assembled using Trinity (v2.15) software to construct the unigene library. Transcript abundance was quantified using Salmon (v1.9.0) by calculating TPM (Transcripts Per Kilobase Million). Differential gene expression analysis was performed using edgeR (v3.40.2) between experimental groups and among individual samples. Functional annotation was conducted against the NR, Swiss-Prot, GO, COG, KOG, eggNOG, and KEGG databases. Differentially Expressed Genes (DEGs) were identified with thresholds set at FDR (False Discovery Rate)< 0.05 and log₂|FC| ≥ 2.

Twelve genes were selected from each comparison for validation by quantitative real-time PCR (qRT-PCR) based on transcriptome data. Expression patterns of petals from three Meconopsis species at five stages (S1–S5; Figure 1A) were analyzed to investigate gene expression dynamics. Total RNA extraction followed the procedure described above. First-strand cDNA was synthesized from total RNA according to the instructions of FastKing RT Kit with gDNA (KR116, Tiangen, China). qPCR was performed with the following reaction parameters: 94°C for 20 s, 40 cycles of 94°C for 10 s and 60°C for 20 s, and 60C for 30 s. A 10 μL reaction system was used as follows: 1 μL cDNA template, 5 μL qPCR Master Mix (Lanyun, China), 0.2 μL forward primer, 0.2μL reverse primer, and 3.6 μL nuclease-free water. GAPDH was used as the reference gene for normalization (Wang et al., 2023). Primers were designed using Primer Premier 6 software. 2^-ΔΔCT method was used to normalize the relative expression of the DEGs (Supplementary Table S1). All qRT-PCR experiments were performed in triplicate. The plant material used for qRT-PCR validation was identical to that used in the transcriptomic analysis.

The petal epidermal cells of the three Meconopsis species at the full-bloom stage (S4; Figure 1A) exhibited similar overall morphology, with intact and elongated cell shapes (Supplementary Figure S1). Therefore, cell morphology in Meconopsis petals appeared to have no significant effect on flower coloration. The petal hues of the three Meconopsis species varied across three developmental stages (Table 1). In M. balangensis (Mb), L* values were 47.50, 50.57, and 48.16, indicating a change in blue intensity from deep to light and then returning to deep across the three developmental stages. The a* value of M. punicea (Mp) ranged from 35.29 to 40.55, and the L* value ranged from 34.21 to 44.58. In M. integrifolia (Mi), L* values decreased progressively from 86.49 to 79.19, while b* values increased steadily from 29.99 to 60.59 (Figure 1C).

Pigment contents and pH values in the petals of the three Meconopsis species are shown in Figure 1D. In Mb, chlorophyll, carotenoid contents, and pH values decreased throughout flower development. Meanwhile, flavonoid and total anthocyanin levels first declined and then increased. In Mp, carotenoid, flavonoid, total anthocyanin contents, and pH values gradually decreased during flower development, whereas chlorophyll decreased initially and then increased. Total anthocyanin content in M. punicea was significantly higher than in the petals of the other two Meconopsis species. In Mi, chlorophyll, carotenoid, flavonoid, and total anthocyanin contents gradually decreased throughout flower development, whereas pH values exhibited the opposite trend. Petals of Mi contained significantly higher flavonoid levels than those of the other two Meconopsis species.

Correlation analysis between color indices and pigment contents across the three developmental stages revealed significant relationships among the three species (Supplementary Table S2). In Mb and Mp, L* values exhibited significant negative correlations with flavonoid and total anthocyanin contents in both blue and red flowers, indicating that higher pigment concentrations corresponded to darker floral coloration. Moreover, carotenoid content displayed a strong positive correlation with b* values in Mp (P < 0.01), suggesting that reduced carotenoid levels might contribute to the decline in b* values. In Mi, b* values showed a strong negative correlation with pigment contents (P < 0.01). Furthermore, Mi exhibited significantly higher flavonoid content than the other two Meconopsis species, suggesting that specific flavonoid compounds may contribute to yellow petal coloration. Collectively, these findings highlight the pivotal roles of flavonoids and total anthocyanins in determining Meconopsis flower coloration.

A total of 847 metabolites were identified in the petals of Ma, Mb, Mp and Mi. The classification and quantitative distribution of these metabolites are shown in Supplementary Figure S2. The major metabolites included lipids, organic acids, phenolic acids, and flavonoids. Among them, 53 flavonoid metabolites were identified. Flavonols, flavones, and anthocyanins were the most abundant subclasses, accounting for 53%, 19%, and 9% of total flavonoids, respectively. In the significantly enriched pathways (Figures 2A–C), using Ma as the control (CK), floral pigment-related pathways in Mb and Mp were mainly enriched in flavonoid biosynthesis (ko00941). Although anthocyanin-related pathways were not significantly enriched, anthocyanin-derived differential metabolites accumulated at high levels in Mb and Mp petals, suggesting a potential role in floral coloration.

In the comparison between Mb and Ma, seven and three differentially accumulated metabolites (DAMs) related to flavonoids and anthocyanins were identified, respectively (Figure 2D). Several anthocyanins were significantly upregulated, including cyanidin-3-sambubioside, delphinidin-3-sambubioside, and delphinidin-3-O-sophoroside, with fold changes (FCs) of 70.08, 12.72, and 3.30, respectively. As precursors in anthocyanin biosynthesis, dihydroquercetin and leucodelphinidin were also significantly upregulated, with high fold changes of 16.50 and 4.22, respectively.

In the comparison group between Mp and Ma, six and two DAMs were enriched in the flavonoid and anthocyanin biosynthesis pathways, respectively (Figure 2E). The levels of quercetin and kaempferol were downregulated, with fold changes of 22.14 and 18.60. Dihydroquercetin, a key intermediate in anthocyanin glycoside biosynthesis, and anthocyanin showed significant upregulation. Cyanidin-3-sambubioside, dihydroquercetin, and cyanidin-3-O-glucoside exhibited fold changes of 52.60, 29.01, and 6.78, respectively.

In comparison, Mi showed enrichment in flavonoid biosynthesis and flavone/flavonol biosynthesis (ko00944), with eight and four DAMs involved in these pathways, respectively (Figure 2F). Four metabolites were downregulated, namely dihydromyricetin, kaempferol, kaempferol-3-O-glucoside, and kaempferol-3-O-sophoroside, with fold changes of 14.11, 21.17, 114.43, and 9.64, respectively. Among the upregulated metabolites, dihydroquercetin had the highest fold change at 114.07, followed by quercetin-3-O-sophoroside at 108.31. Naringenin chalcone, an intermediate in flavonol biosynthesis, also showed an upregulation trend, with a fold change of 5.18.

RNA-sequencing (RNA-seq) was used to analyze gene expression profile changes and understand the molecular mechanisms underlying different flower colors. As Meconopsis lacks a reference genome sequence, the transcript sequences assembled by Trinity were utilized as the reference for subsequent analyses. With three biological replicates, a total of 498,759,980 clean reads (representing 73.05 GB of clean data) were generated from 12 petal samples (Supplementary Table S3). In total, 569,449 transcripts and 122,876 unigenes were obtained (Supplementary Table S4). To annotate these unigenes, sequence comparisons were performed against multiple databases, including GO (34.37% of unigenes), KEGG (14.61%), Pfam (27.20%), Swiss-Prot (27.67%), eggNOG (38.44%), NR (51.52%), and transcription factors (TF, 1.99%) (Supplementary Table S5). PCA score plot of mass spectrometry data for each sample confirmed that the experimental procedures were reproducible and suitable for subsequent analyses (Figure 3A).

Using Ma as a control, differentially expressed genes (DEGs) were selected based on the criteria of |log₂Fold Change| ≥ 1 and FDR< 0.05. Venn diagrams were constructed for the differentially expressed genes in each comparison group (Figure 3B). Furthermore, the total number of DEGs, upregulated genes, and downregulated genes was calculated for each comparison (Figure 3C). In the Mb vs Ma comparison group, 26,738 upregulated and 23,165 downregulated DEGs were observed. In the Mp vs Ma comparison, the numbers of upregulated and downregulated DEGs were 28,552 and 22,718, respectively. The Mi vs Ma comparison identified 45,613 DEGs, with 22,369 upregulated and 23,244 downregulated, respectively.

With Ma as the control, the KEGG enrichment analysis of DEGs in the three comparison groups is shown in Figures 3D–F. DEGs were significantly enriched in pathways such as flavonoid biosynthesis (ko00941), circadian rhythm (ko04712), and plant hormone signal transduction (ko04075) across all three comparison groups. DEGs in Mp were significantly enriched in the anthocyanin biosynthesis pathway. In contrast, the comparison between Mi and Ma showed specific enrichment in the flavone and flavonol biosynthesis pathway (ko00944). These pathways, including flavonoid biosynthesis (ko00941), anthocyanin biosynthesis (ko00942), and flavonol biosynthesis (ko00944), were recognized as critical for regulating petal pigmentation.

Combined metabolomic and transcriptomic analyses revealed that Mb, Mp and Mi was significantly enriched in the flavonoid biosynthesis pathway. The flavone and flavonol biosynthesis pathway was also identified in Mi. The unigenes involved in the flavonoid biosynthesis pathway were screened from the RNA-seq data set. The expression profiles of flavonoid biosynthesis pathway structural genes in the different colored petals based on their TPM values were illustrated using a heatmap analysis. Building upon existing research in the flavonoid biosynthesis pathway, a heatmap of DEGs of Mb, Mp and Mi has been generated (Figures 4A, 5A and 6A) (Qu et al., 2022; Chen et al., 2024; Wang et al., 2024; Kong et al., 2025; Ni et al., 2025). qRT-PCR analysis was performed for 15 genes to explore the expression patterns of key DEGs at five stages of flower development in three species (Figures 4B, 5B, 6B). The qRT-PCR results of the DEGs showed the same trend as the RNA-Seq results, indicating the high reliability of the data obtained by transcriptome sequencing (Supplementary Figures S5–S7). Correlation analyses were also conducted between the relative expression levels of key genes at three floral developmental stages and the contents of flavonoids and total anthocyanins.

A total of 76 structural genes from 11 gene families involved in anthocyanin biosynthesis were identified in the Mb genome. Among these, ten PALs, two C4Hs, five 4CLs, three CHSs, four CHI, three F3Hs, one F3’Hs, four DFRs, and two ANSs genes showed significant upregulation in Mb. Among the late biosynthetic genes, DFR2 and DFR4 were not expressed in Ma but were highly expressed in Mb. ANS1 and ANS2 were upregulated by 5.58- and 5.00-fold, respectively. In contrast, UFGT genes were expressed at low levels in Mb, despite the significant accumulation of their catalytic products, cyanidin glycoside and delphinidin glycoside. To further examine their temporal expression dynamics, gene expression in Mb petals was analyzed across five floral developmental stages. UFGT1 and UFGT2 showed peak expression at early bud stage (S1). This suggests that UFGT activity is temporally regulated — functioning o during early bud differentiation to promote anthocyanin accumulation, followed by reduced expression as floral organs mature and pigmentation stabilizes (Figure 4B). Pearson correlation analysis between gene expression and anthocyanin content across developmental stages revealed that PAL6, F3’H5, DFR3, ANS2, UFGT1, and UFGT2 were significantly positively correlated with total anthocyanin content (Supplementary Table S9), suggesting their potential roles in promoting anthocyanin biosynthesis and petal coloration in Mb.

A total of 34 differentially upregulated genes and 28 differentially downregulated genes were identified in Mp vs Ma. Among these, four PALs, one C4H, four 4CLs, four CHSs, three CHIs, three F3Hs, two F3’Hs, three DFRs, and three ANSs showed significant upregulation in Mp, thereby positively regulating the synthesis of the pigmented compound cyanidin glycosides. As F3’H, DFR, and FLS were located at the branching positions of anthocyanin biosynthesis mentioned above, their expression specificity deserved special attention to unveil the molecular mechanisms underlying spatial anthocyanin biosynthesis in Mp. Dihydromyricetin and kaempferol, catalyzed by F3’5’H and FLS respectively, showed significant decreases, whereas dihydroquercetin derived from F3’H accumulated substantially in Mp. Consequently, metabolic flux was redirected toward anthocyanin biosynthesis.

To gain deeper insights into the spatiotemporal expression patterns of these genes, the relative expression levels in Mp petals were examined at five successive flowering stages. Most of the genes’ expression levels exhibited a pattern of first decreasing, then increasing, and finally decreasing again. These genes showed high expression at S1 stage and were significantly downregulated at S2 stage (Figure 5B). Pearson’s correlation analysis showed that the expressions of ANS1, DFR3, DFR6, F3H6, F3’H2, F3’H6, F3’H7, CHI8, CHS4, UFGT2 and UFGT4 were significantly positively correlated with total anthocyanin accumulation (Supplementary Table S10), suggesting that these genes may promote anthocyanin biosynthesis.

A total of 36 up- and 19 downregulated genes were detected in Mi vs Ma. The upregulated genes included nine PALs, two C4Hs, five 4CLs, five CHSs, four CHIs, one F3H, one F3’H, and three FLSs genes that showed significant upregulation in Mi, thereby positively regulating the synthesis of quercetin glycosides. F3’5’H, FLS, DFR, and F3’H competed for the substrate dihydrokaempferol. DFR1 showed low expression levels in Mi, while F3’H4 had a relatively large log₂FC of 2.88. FLS14, FLS17, and FLS18 were upregulated by 4.12-fold, 11.94-fold, and 12.17-fold, respectively. The strong expression of FLS directed the metabolic flux toward quercetin, which was further glycosylated into quercetin glycosides.

To further elucidate the temporal expression dynamics of these genes, their expression patterns were analyzed across five floral developmental stages in Mi. Expression levels of F3H1, F3H9, FLS17, FLS18, and UFGT5 showed an upward trend during floral development, with low expression from S1 to S3 stage and high expression at S4 stage (Figure 6B). In addition, these genes showed a significant negative correlation with flavonoid content. (Supplementary Table S11). Given that the yellow color of Mi petals was primarily determined by quercetin derivatives among flavonoids, the expression of these genes showed a synchronous trend with the gradual increase in the yellowness b* value during the flowering period. It is thus hypothesized that these genes may exert a critical function during the yellow flower development of Mi.

Transcription factors (TFs) were predicted using the PlantTFDB website and integrated with transcriptome annotation, leading to the identification of a total of 54 classes of differentially expressed TFs. The top five families with the highest number of members are shown in Supplementary Figure S4, including the ERF, MYB, bHLH families. MYB and bHLH were the transcription factor families most frequently involved in flower color research. The heatmaps of genes encoding these two transcription factor families were shown (Figures 7A, B). Comparative analysis using Ma as the control revealed differential expression of MYB and bHLH genes across the three species: Mb (42 MYBs, 27 bHLHs), Mp (44 MYBs, 26 bHLHs), and Mi (38 MYBs, 36 bHLHs). In each of the three Meconopsis species, two differentially expressed MYB and two bHLH genes were identified. Their relative expression levels were measured across five floral developmental stages (Figures 7C–E). Correlation analyses were performed between gene expression and the contents of flavonoids and total anthocyanins (Supplementary Tables S9–S11). Results indicated that MbbHLH1, MbMYB30 and MpbHLH19 exhibited significant positive correlations with total anthocyanin content, implying a positive regulatory role in anthocyanin synthesis and floral pigmentation. MiMYB1, MiMYB30, MibHLH2 and MibHLH19 were negatively correlated with flavonoid content, while their expression trends matched the progressive elevation of yellowness b* value during flowering, which suggests their critical function in yellow flower development.

The results of this study revealed that petal coloration in Meconopsis is primarily governed by variations in pigment composition and petal pH. In M. balangensis (Mb), the significant correlation between L* and b* values, but not a* values, indicates that lightness is mainly affected by petal blueness. The significant positive correlation among the L* value, b* value, flavonoids and total anthocyanins indicates that these substances are the major determinants of blue petal pigmentation, which is consistent with the findings of previous studies (Zan et al., 2024). In Primula vulgaris, Petunia hybrida and Pueraria lobata, blue or purple flower morphs consistently exhibit higher petal pH values than red morphs (Quattrocchio et al., 2006; Tatsuzawa et al., 2017; Zhai et al., 2020). The petal pH of M. balangensis is higher than that of M. punicea, potentially due to the stability of anthocyanins, which retain red coloration at lower pH but shift toward blue and become unstable at higher vacuolar pH levels (Yoshida et al., 2010). The blue pigment in M. grandis is likely a novel type of metal complex pigment. Researchers successfully reproduced a comparable blue hue by combining anthocyanins, flavonols, and metal ions in a buffered solution at pH 5.0 (Yoshida et al., 2006; Qu et al., 2022). Given the critical role of petal pH in blue coloration in Meconopsis, future research should focus on elucidating the regulatory mechanisms of pH-related genes.

In M. punicea (Mp), the high anthocyanin content was strongly and positively correlated with the a* (redness) value, consistent with earlier studies in Paeonia suffruticosa (Luo et al., 2021). These results indicate that total anthocyanin concentration is the primary factor contributing to red coloration. Anthocyanins display stable red coloration under low-pH conditions, and changes in their stability directly contribute to floral color variation (Tanaka et al., 1998). In M. punicea, a significant positive correlation was observed among a*, pH, and total anthocyanin content, suggesting that pH may affect red coloration by modulating anthocyanin stability (Yu et al., 2024). In M. punicea, carotenoid content was strongly positively correlated with the b* (yellowness) value, indicating that reduced carotenoid levels may lower b* values, consistent with observations in Edgeworthia chrysantha (Zhou et al., 2023). Variations in carotenoid content may reduce petal yellowness and result in subtle changes in floral coloration in M. punicea. Previous studies on M. punicea suggest that carotenoids may play a regulatory role in flower coloration (Qu et al., 2022).

In M. integrifolia (Mi), lightness (L*) was positively correlated with flavonoid content, while yellowness (b*) showed a significant negative correlation (P < 0.01). Flavonoid content was significantly higher than that in the other two species, whereas anthocyanin content was comparatively lower. Flavones and flavonols have been shown to impart white to pale yellow coloration to petals (Lin et al., 2021). Quercetin derivatives, a class of flavonols, have been reported as the major yellow pigments responsible for the floral coloration in Camellia nitidissima and Osmanthus fragrans (Zhou et al., 2013; Zou et al., 2017). Therefore, the high accumulation of specific flavones and flavonols may contribute to the yellow petal coloration in this species. The petal color of Camellia reticulata deepens progressively, accompanied by a gradual decrease in pH (Xue et al., 2015). Compared with M. balangensis and M. punicea, the petals of the light-colored species M. integrifolia exhibit a higher pH, which may enhance the stability of yellow pigments (Yoshida et al., 2010).

Flavonoids were identified as the central pigment group responsible for color diversity in Meconopsis. In blue flowers of M. balangensis, high accumulation of cyanidin-3-sambubioside, delphinidin-3-sambubioside, and delphinidin-3-O-sophoroside was detected, consistent with reports that delphinidin derivatives confer blue coloration in M. horridula and M. betonicifolia (Tanaka et al., 2001). Flavones and flavonols act as copigments with chromogenic anthocyanins, thus facilitating the bluing or deepening of floral coloration (Mizuno et al., 2013). The copigment-induced enhancement of blue coloration has been documented in M. horridula, M. betonicifolia, Torenia fournieri and Dahlia variabilis (Aida et al., 2000; Tanaka et al., 2001; Ayumi et al., 2013). Luteolin (a flavone) and myricetin (a flavonol), both significantly accumulated in M. balangensis, may function as copigments that enhance the coloration effect of delphinidin glycosides, thereby contributing to the blue hue of the petals.

Red petal coloration in M. punicea was mainly associated with the accumulation of cyanidin glycosides, especially cyanidin-3-glucoside and cyanidin-3-sambubioside, in agreement with findings in Camellia japonica and Brassica napus (Li et al., 2019; Ye et al., 2022). In contrast, yellow pigmentation in M. integrifolia resulted from the presence of quercetin derivatives. Quercetin-derived compounds have been identified as the yellow pigments responsible for floral coloration in a variety of plant species, such as Camellia nitidissima and Paeonia spp (Zhou et al., 2013; Yang et al., 2020).

High expression levels of key genes in the flavonoid metabolite pathway promote the production of different floral pigments, which has been investigated in Lysimachia arvensis, Camellia sinensis, and Rosa multiflora (Luo et al., 2015; Kipkoech et al., 2021; Mercedes et al., 2021). Integrated transcriptomic and metabolomic analyses revealed that the three Meconopsis species share a conserved flavonoid biosynthetic framework, yet differ in the regulation of key structural genes and transcription factors. In M. balangensis and M. punicea, high expression of F3Hs, F3’Hs, DFRs and ANSs directed metabolic flux toward anthocyanin biosynthesis, producing blue and red pigments. In Paeonia lactiflora, key structural genes such as ANS, DFR, F3H and UFGT are highly expressed at the early flowering stage and decrease at full bloom, mirroring the trend of total anthocyanin content (Zhao et al., 2012). This expression pattern resembles that of UFGT in M. balangensis at different floral developmental stages observed in this study. High expression levels of FLS and UFGT promoted flavonol biosynthesis, leading to quercetin accumulation and yellow pigmentation in M. integrifolia, and these observations match earlier findings in M. integrifolia and Dasiphora (Chen et al., 2024; Tian et al., 2025).

The MYB, bHLH, and WD40 transcription factors form the MBW complex, which can activate or repress the expression of structural genes, thereby regulating flavonoid metabolism (Hichri et al., 2011; Nakatsuka et al., 2012). Studies in various species, including Aglaonema commutatum, Dendrobium officinale, and Gentiana triflora, have shown that MYBs and bHLHs bind to the promoters of structural genes such as CHSs and DFRs, either independently or synergistically, to activate gene expression and enhance anthocyanin biosynthesis (Nakatsuka et al., 2012; Li et al., 2022; Yang et al., 2023). Notably, their overexpression can also repress DFRs expression and reduce anthocyanin accumulation (Filyushin et al., 2023). In this study, MYBs and bHLHs showed significant correlations with the expression of key structural genes (Supplementary Tables S9-S11). In M. balangensis and M. punicea, MYBs and bHLHs may promote anthocyanin accumulation by upregulating the expression of F3Hs, F3’Hs, DFRs, and ANSs. In contrast, in M. integrifolia, these transcription factors may facilitate flavonol accumulation by enhancing the expression of CHS2, F3H1, F3H9, F3’H4, FLS17, FLS18, and UFGT5, or by repressing DFR1 expression, thereby contributing to yellow flower pigmentation.

A regulatory network diagram depicting the molecular mechanisms governing pigmentation in these three species was developed (Figure 8). The formation of the three flower colors in Meconopsis is fundamentally driven by the flavonoid metabolic pathway. The coordinated action of structural genes (DFR, FLS, UFGT) and transcription factors (MYB, bHLH) shapes the biosynthetic direction toward anthocyanin- or flavonol-dominated pigmentation. This integrated understanding not only elucidates the molecular basis of petal color diversification in Meconopsis but also provides genetic targets for future molecular breeding and pigment engineering in alpine ornamental plants.