Effects of short-term environmental stresses on the onset of cannabinoid production in young immature flowers of industrial hemp (Cannabis sativa L.)
Institute of Cannabis Research, Colorado State University–Pueblo, 2200 Bonforte Blvd., Pueblo, CO 81001 USA
Department of Biology, Colorado State University–Pueblo, 2200 Bonforte Blvd., Pueblo, CO 81001 USA
Department of Chemistry, Colorado State University–Pueblo, 2200 Bonforte Blvd., Pueblo, CO 81001 USA
Abstract
Backgrounds
Cannabis sativa L. produces at least 120 cannabinoids. Although genetic variation is the main factor in cannabinoid production, the effects of short-term environmental stresses in the early flowering stage remains largely unknown.
Methods
To investigate the effects of short-term environmental stresses on the onset of cannabinoid production in young immature flowers, a hemp variety, Green-Thunder (5–8% CBD/mg of dry weight), was treated with mechanical damage, insect herbivory, extreme heat, or drought stress for 5–7 days during the first 2 weeks of flowering. Three hemp tissues, including flowers, leaves, and stems, were collected from hemp grown under these stress conditions at multiple time points during the first 2 weeks after transition to the short photoperiod and analyzed using high pressure liquid chromatography to quantify phytocannabinoids including cannabigerolic acid (CBGA), cannabigerol (CBG), cannabidiolic acid (CBDA), cannabidiol (CBD), Δ-tetrahydrocannabinolic acid (THCA), Δ-tetrahydrocannabinol (THC), and cannabinol (CBN).
Results
The 5 days of mechanical wounding did not affect the production of any of the cannabinoids during the initial stage of flowering. However, after 5 days of herbivore treatment, there was a significant difference in concentration between day 1 and day 6 of CBGA (control: 308 μg/g; treatment – 24 μg/g), CBG (control: 69 μg/g; treatment: 52 μg/g), and CBD (control: 755 μg/g; treatment: 194 μg/g) between the control and treatment plants. The 7 days of heat treatment at 45–50 oC significantly reduced the production of CBGA during this observed window (control: 206 μg/g; treatment: 182 μg/g) and CBG (control: 21 μg/g; treatment: − 112 μg/g). Notably, the largest change was observed after 7 days of drought stress, when plants showed a 40% greater accumulation of CBG (control: 336 μg/g; treatment: 622 μg/g), and a significant decrease (70–80%) in CBD (control: 1182 μg/g; treatment: 297 μg/g) and THC amounts (control: 3927 μg/g; treatment: 580 μg/g).
Conclusions
Although this observation is limited in the early flowering stage, the common field stresses are adequate to induce changes in the cannabinoid profiles, particularly drought stress being the most impactful stress for hemp flower initiation with the altering the cannabinoid production by decreasing CBD and THC accumulation while increasing CBG by 40%.
Supplementary Information
The online version contains supplementary material available at 10.1186/s42238-021-00111-y.
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Keywords: Cannabis sativa, Cannabinoids, CBD, THC, Abiotic stress, Biotic stress, Secondary metabolites
Article notes
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Received 2020 Apr 2; Accepted 2021 Nov 23; Collection date 2022.
Introduction
Plants produce secondary metabolites that play important roles in plant adaptation and survival under stress conditions along with primary metabolites that are essential for their growth and development (Ramakrishna and Ravishankar 2011). Often, the secondary metabolites confer specific odors, colors, and tastes in plants. Plant secondary metabolites have been widely used as sources for food additives, flavors, cosmetics, industrial biochemicals, and biopharmaceuticals (Gonçalves et al. 2019; Ramakrishna and Ravishankar 2011).
Cannabis sativa L., a member of the Cannabaceae family, is a primarily annual, dioecious variety that produces secondary metabolites called cannabinoids (Elsohly and Slade 2005; White et al. 2016). Cannabis produces at least 120 different cannabinoids which are synthesized in the basal disk cells and stored in the secretory cavity in glandular trichomes (Ebersbach et al. 2018; Livingston et al. 2020). The different cannabinoid carrying capacity observed in Cannabis is largely dependent on the number of trichomes (Kim and Mahlberg 1997; Livingston et al. 2020). Flower tissues have the highest concentration of glandular trichomes, which corresponds to this tissue showing the greatest amounts of cannabinoids. Two major cannabinoids are (-)-Δ9-trans-tetrahydrocannabinolic acid (Δ9–THCA) and cannabidiolic acid (CBDA) that are synthesized from a common precursor, cannabigerolic acid (CBGA), by THCA and CBDA synthase respectively, and then can be decarboxylated into CBD and THC through various processes, such as heating, light exposure, or through chemical reactions (Chandra et al. 2017; Wang et al. 2016).
Over the past years, Cannabis plants, especially its chemical derivatives cannabinoids, have regained public attention due to their therapeutic potentials in Dravet and Lennox-Gastaut syndrome, Parkinson’s disease, cancers, mental illnesses, and other neurological disorders (Montoya et al. 2020; Pauli et al. 2020). In the 2018 Farm Bill, hemp has been reclassified as an agriculture commodity. To meet increased demands, a great deal of selective breeding efforts has been made to develop elite varieties with various cannabinoid profiles and new dominant cannabinoids (de Meijer and Hammond 2005; de Meijer et al. 2009a, b; Williamson 2004). Furthermore, yeast has successfully been genetically engineered as an alternative cannabinoid production platform (Luo et al. 2019).
The phytocannabinoid content of Cannabis is primarily determined by genetic factors that are inheritable and differentially expressed dependent on variety, tissue type, position of tissue, and the growth stage (Chandra et al. 2013; Kovalchuk et al. 2020; Namdar et al. 2018). In addition, environmental conditions are the other major factors that contribute to the production and accumulation of cannabinoids (Gorelick and Bernstein 2017). Like other crops, the production of cannabinoids, especially THC and CBD, are also greatly affected by a variety of environmental stresses such as light (Eichhorn Bilodeau et al. 2019; Magagnini et al. 2018), temperature (Gorelick and Bernstein 2017), water deficit (Caplan et al. 2019; Gorelick and Bernstein 2017), nutrition (Bernstein et al. 2019a, Gorelick and Bernstein 2017), heavy metals (Husain et al. 2019), phytohormones (Burgel et al. 2020), soil bacteria (Pagnani et al. 2018), and biotic stresses including insect and microbial pathogens (Langenheim 1994; McPartland et al. 2000; Sirikantaramas et al. 2005). Environmental stresses cause numerous plant-wide responses, which are classified into three types: (1) systematic acquired resistance to pathogens (Fu and Dong 2013), (2) systematic wound responses to damage and herbivory (Savatin et al. 2014), and (3) systemic acquired acclimation to abiotic stresses (Mittler and Blumwald 2015). A recent study shows that traits like the number of days to maturity as well as THC and CBD production are strongly determined entirely by genetic factors, whereas traits such as plant height, grain yield, and water usage were influenced by environmental factors and the interaction between genetic and environmental factors (Campbell et al. 2019).
Abiotic factors or elicitors include photon-radiation, nutrient deficiency, heavy metal presence, drought, and temperature stress (Gorelick and Bernstein 2017). Cannabis plants have evolved in high irradiation environments which plays a critical role in leaf morphology and the production of cannabinoids (Magagnini et al. 2018). Magagnini et al. 2018 showed that Cannabis grown under blue wavelength (~ 450–520 nm) with a short photoperiod (12 h light/12 h dark) yielded the highest CBD and THC accumulations. Also, the blue light spectrum induced a greater amount of cannabigerol (CBG) when combined with UV-A light (Eichhorn Bilodeau et al. 2019; Magagnini et al. 2018). This was also supported by a more recent study, where the authors observed the greatest cannabinoid production change by blue-rich light spectrums, specifically observing CBGA accumulation stimulation when comparing to far-red lights (Danziger and Bernstein 2021a). In long-day plants, flowering is mostly promoted by red (R, ~ 625–700 nm) and far-red (FR, > 700 nm) lights which is delivered during the early and later parts of the photoperiod, respectively (Backer et al. 2019; Eichhorn Bilodeau et al. 2019). However, the response of CBDA, THCA, and CBCA to light spectrum appeared to be cultivar-specific (Danziger and Bernstein 2021a). Some Cannabis genotypes such as “G-170” appeared to be insensitive to changes in the R:FR, showing no effect on flowering in response to the changes in R:FR ratio (Magagnini et al. 2018). The same study additionally showed that the light insensitive Cannabis has an increased development of mature cuttings when exposed to the low R:FR ratio during a long photoperiod (18 h light/6 h dark) (Magagnini et al. 2018).
In addition, temperature is an important factor for canopy formation in fiber hemp. A study showed that the rate of leaf appearance and stem elongation linearly increased as temperature rises from 10 oC to 28 oC (Van Der Werf et al. 1995). Due to global warming, agricultural crops including Cannabis plants encounter multiplexed environmental stresses of which extreme heat and drought are the most impactful. Herppich et al. 2020 showed that two fiber-type hemp varieties (‘Santhica 27’ and ‘Ivory’) responded differently against the combined stress. ‘Santhica 27’ utilized low CO2 uptake rates in lower leaves and higher seed germination rates that resulted in twice the fiber yield compared to ‘Ivory’, whereas ‘Ivory’ developed high rates of CO2 gain which enabled the establishment of large leaf area with more stomatal regulation, resulting in higher water use efficiency (Herppich et al. 2020). As seen in this study, fiber hemp promptly reprogramed their photosynthetic rate, transpiration, stomatal regulation, and water use efficiency upon treatment of environmental stresses, affecting the yield performance, which affects the total content and potentially the ratios of secondary metabolites in Cannabis.
Another recent study demonstrated that drought stress significantly alters gene expression patterns (Gao et al. 2018). Through analyzing differential gene expression of drought stress compared to a control group, it appears there were 55 differentially expressed genes that are responsible for secondary metabolite biosynthesis in response to drought conditions, as well as the genes involved in the ABA induction and its signal transduction pathway; however, chemical concentrations were not measured to identify if the observed gene expressions differences affected secondary metabolite production (Gao et al. 2018).
Mineral nutrient supplements can impact cannabinoid profiles as well. It has been reported that the supplementation of mineral nutrients (e.g., nitrogen, calcium, iron, and magnesium) increased cannabinoids production, although others have reported that nutrient deficiencies may stimulate the cannabinoid production as well (Gorelick and Bernstein 2017). A study showed that phosphorus enhanced fertilizer increases the level of CBD, CBG, CBN while decreasing THC by 16% (Bernstein et al. 2019a). A more recent study in 2021 demonstrated the dose-dependent effects of phosphorus in cannabinoid biosynthesis as well as plant functional-physiology, which affects the pharmacological quality of cannabinoids (Shipony and Bernstein 2021). Another key nutrient, nitrogen, also significantly affected the Cannabis chemical profile. A recent study showed that the highest concentrations of cannabinoid and terpenoids were highest under the 30 mg/L of nitrogen and reduced with the increase of nitrogen supply (Saloner and Bernstein 2020). Three inorganic nutrients, nitrogen, phosphorus, and potassium, supplemented with humic acids significantly increased the level of CBG by 71% in flowers while lowering CBN levels by 38% and 36% in both flowers and inflorescence leaves, respectively (Bernstein et al. 2019a). Heavy metals can also affect plant physiology and molecular mechanisms. Cannabis plants are tolerant to moderate concentration of cadmium (Linger et al. 2005), nickel, and chromium (Citterio et al. 2005), with no major effects on growth and development (Gorelick and Bernstein 2017). A recent study indicated that six industrial hemp varieties grown on the abandoned coal mine soil in Pennsylvania had a significant increase level of total CBD content when compared to those grown in a commercial soil while the seed germination rates and plant height were not affected (Husain et al. 2019).
Additionally, phytohormones are important growth regulators which play an important role in the plant cellular processes, metabolism, growth, and plant defense responses against stresses (Egamberdieva et al. 2017, Gorelick and Bernstein 2017). Physical stressors (e.g., rainstorms, hailstorms, herbivory, and mechanical damages from agricultural equipment) generally found in hemp fields induce signal molecules such as jasmonic acid (JA), ABA, systemin, and oligogalacturonides, alerting both adjacent and remote tissues to activate mechanisms required for healing and further defense (Leon et al. 2001). Upon receiving a signal molecule, various enzymatic pathways are modulated to alter contents of bioactive metabolites such as terpenoids, alkaloids, and phenylpropanoids (Chandra et al. 2017).
To elucidate the roles of endogenous hormones, a Cannabis suspension cell culture was used to study the application of JA and salicylic acid (SA). The results showed no significant changes in cannabinoid content, which might be due to the limited amount of cannabinoid production in the cell culture system (Flores-Sanchez et al. 2009; Peč et al. 2010). However, a study performed on drug-type Cannabis plants with a abscisic acid (ABA) treatment showed the reduction of CBD and THC levels during vegetative stage (Mansouri and Asrar 2012) while increased THC was observed in leaves and flowers in male plants (Mansouri et al. 2009; Mansouri and Asrar 2012).
Several studies also reported that exogenously applied plant growth regulators have an impact on morphology, flower biomass, and cannabinoid contents of Cannabis sativa L. (Burgel et al. 2020; Lalge et al. 2016). A study showed that the plant architecture (e.g., height, length of axillary branches, and number of internodes) was significantly reduced by the treatment of synthetic auxin (1-naphthalenaecetic acid; NAA), cytokine (6-benzylaminopurine; BAP), and a mixture of both, when compared to the untreated control plants (Burgel et al. 2020). It is noted that BAP reduced height and number of internodes but the length of axillary branches were not affected. These exogenously applied growth regulators on the hemp variety ‘KANADA’ have aided in the uniform and compact growth of the plants, as well as enabled higher CBD production in indoor growth conditions (Burgel et al. 2020).
Other than aforementioned environmental factors, hemp biomass yield and cannabinoid production can be also influenced by various agronomical practices such as plant density, sowing time, cropping system (García-Tejero et al. 2019), plant architecture (Danziger and Bernstein 2021b), and geographical location (Aubin et al. 2016).
Similar to abiotic stresses, biotic stresses also cause metabolite concentration changes. Hemp plants are susceptible to a variety of insects. Nearly 300 insect pests have been reported but only a few are known to cause economic loss (McPartland 1996). In hemp plants, the most serious pests are lepidopterous stem borers including European corn borers (Ostrinia nubilalis) and hemp borers (Grapholita delineana) (McPartland 2002). Comparing to other field crops, hemp is relatively pest-tolerant plants because of the pest-repellent properties of cannabinoids and terpenoids present (Dambolena et al. 2016). Recent studies have demonstrated that cannabinoid-enriched extracts show pesticidal activity to defend themselves from insect herbivore attacks (Benelli et al. 2018; Park et al. 2019a). Although the impacts of insect damage on cannabinoid content is not well documented, the increase in biomass and seed productivity were observed in hemp resulting from branch proliferation caused by European corn borer (Small et al. 2007). It is also reported that phytocannabinoid concentration and composition was significantly correlated to structure of endorhiza communities (Winston et al. 2014).
The aim of this study is to investigate if commonly reported biotic and abiotic stresses, including mechanical damage, insect damage, excess heat, and drought stress, influence cannabinoid production and bioaccumulation of a local Colorado hemp variety (Cannabis sativa L.) during the early flowering stage under semi-controlled environment. Better understanding on the environmental effects of cannabinoid production would be a necessary step for a successful hemp cultivation.
Materials and methods
Cannabis cultivation and cloning
For cannabinoid analysis, the local Colorado hemp variety that is known to produce around 5–10% CBD, named Green-Thunder, was grown in a greenhouse maintained at 20–25 oC under a 16 h light/8 h dark cycle at a humidity level of 50–70%. A single female hemp plant was used to generate multiple clones that provided similar cannabinoids levels. To produce clones, an apical meristem with at least one set of fan leaves were taken from the mother plant and treated with Clonex rooting gel (Growth Technology Ltd., Somerset, UK) containing indole-3-butyric acid, then placed into a rapid rooter, which is a moist compressed coconut/peet cube (3 cm length × 3cm width × 5cm height). The cubes were maintained in a hydroponic system (38 cm length × 30 cm width × 26 cm height) that is filled with the root induction solution containing 12 L deionized water blended with 31 ml of Botanicare Liquid Karma (Botanicare, Vancouver, WA) under T5 fluorescent light bulbs (432 W, 242 μmol/m2/s) until the roots reached 15–20 cm long. The rooted clones were transplanted into 25 cm square pots filled with Pro-Mix HP soil (PRO-MIX, Quakertown, PA) and acclimated for a week. Then, the clones were moved to a grow tent (2 m length × 1.5 m width × 2 m height) maintained at 20–25 oC at a humidity level of 50–70% under 16 h light/8 h dark cycle during vegetative stage for 6 weeks and then into a 12 h light/12 h dark cycle to induce the flowering stage and simulate each different stress condition. The hemp plants were irrigated with 1 L of water at twice weekly, except for drought treatment (200 ml).
Stress treatments
For our stress experiment, a total of 12 hemp clones were taken from a 2-month-old mother plant forced to remain at a vegetative stage with 24 h light cycle under AgroBrite T5 fluorescent light bulbs (432 W, 242 μmol/m2/s) (Hydrofarm, Denver, CO). The height of the mother plant was controlled by cutting apical and lateral meristems at around 1 m tall. Six untreated control plants were grown under the semi-controlled grow tent (2 m length × 1.5 m width × 2 m height) maintained at 20–25 oC at a humidity level of 50–70% under 16 h light/8 h dark cycle during vegetative stage for 6 weeks, while the other six plants were grown in a separate grow tent under same conditions except for the given stress. For all the stress tests, 7-week-old hemp clones that are in week 2 of the flowering stage were used. For the mechanical wounding experiment, on day 1, three fully expanded fan leaves, at least three nodes from the top were punctured using a 1/4″ round hole punch for 12 holes per leaf. For the main stem wounding, a blade was used to generate five 1-inch-long vertical incisions on the stalk. The percentage of tissue loss per leaf and stems was maintained at no more than 20%. In a series of wounding introduced in the next 2 days, the remaining lower parts of the plant were treated. For herbivore damage, a total of twenty 3rd instar caterpillar larvae of tobacco hornworm Manduca sexta were placed on the leaves of six hemp plants that were covered with a mesh net bag for 5 days. For the heat treatment, excess heat was generated by a heater that maintained the grow tent at 45–50 oC for 7 days. To prevent the tent from overheating, an additional exhaust fan was installed for better ventilation. For the drought experiment, the water deficient condition was simulated by irrigating twice a week with 200 ml which is approximately 20% relative water content in the soil, while control plants were grown under well-watered condition. Once each treatment was completed, the flower, leaf, and stem tissues were collected separately. Of six hemp plants initially subjected to each stress test, the three most healthy- and representative plants were chosen for cannabinoid analysis. All flowers, leaves, and stems tissues were separately collected, and the sampled tissues were immediately stored on ice and then stored at -80 o C until further analysis.
Analysis of Cannabinoids using high pressure liquid chromatography (HPLC)
The cannabinoid extraction from plant materials was conducted using the United Nations Office on Drugs and Crime (UNODC) method with modifications (UNODC 2009). Samples were weighed to 0.5 g, then extracted with 5 ml of a (9:1, v/v) methanol (MeOH): chloroform solution. The mixture was vortexed before being placed in a sonication bath for 15 min and vortexed every 5 min. The sample was then centrifuged at 4500 rpm for 15 min and then the supernatant was collected and stored in a refrigerator at 4 °C until analysis. Extracts were analyzed by high pressure liquid chromatography (HPLC) on a Dionex UltiMate 3000. Stock standards of cannabigerolic acid (CBGA), cannabigerol (CBG), cannabidiolic acid (CBDA), cannabidiol (CBD), Δ-tetrahydrocannabinolic acid (THCA), Δ-tetrahydrocannabinol (THC), and cannabinol (CBN) were purchased from Cerilliant (Millipore Sigma, St. Louis, MO) in 1mg/ml glass ampules. The stock standard of 100 μg/ml of the cannabinoids was diluted in MeOH which was used to create the calibration curve, where 10 μg/ml, 50 μg/ml, and 100 μg/ml were points on the curve. HPLC analysis included external calibration with each set of samples, solvent blanks, and analysis of independently prepared continuing calibration verification samples every twentieth sample to ensure accuracy. A binary gradient at a flow rate of 0.450 ml/min was used for separation. Mobile phase A was a 0.1% formic acid aqueous solution and mobile phase B consisted of MeOH. Cannabinoids were quantified by absorbance at 210 nm. Chromatographic separation of the cannabinoids was accomplished using an Accucore aQ C18 Polar Endcapped column (100 mm × 2.1 mm, particle size 2.6 μm). Initial conditions: 67% B with a non-linear gradient to 81% B from 0.0 to 8.0 min giving the gradient a concave inflection point near 5.0 min. The remaining gradients were linear. Mobile phase B was increased to 83% at 13.0 min, then increased again to 95% at 16.0 min, and then returned to 67% for 7.0 min of equilibration.
Statistical analysis
The differences in cannabinoid levels in each tissue (n = 3) and the tissue-specific differences over day 7, 12, and 14 during the first 2 weeks of flowering stage were analyzed for statistical significance by one-way ANOVA and two-way ANOVA, respectively, followed by Tukey’s post-test available in the GraphPad Prism software package (GraphPad Software, Inc., La Jolla, CA). Differences between the untreated control and stress-treated groups were considered to be statistically significant at *p < 0.05, **p < 0.01, ***p < 0.001, ****p < 0.0001. All graphs were represented as mean ± standard deviation (s.d.). Concentration values reported are the difference between the concentration on day 1 and the concentration on day 6 or day 8 for each the control and treated plants. A positive value indicates that an increase in that cannabinoid concentration during that timeframe was observed, whereas, a negative value indicates that cannabinoid decreased concentration between days 1 and day 6 or day 8 depending on the treatment.
Results and discussion
Early floral cannabinoid production
To determine the spatial- and temporal-specific cannabinoid production, the amounts of CBGA, CBG, CBDA, CBD, THCA, THC, and CBN in the immature buds, leaves, and stem tissues were quantified and compared. A previous study reported that the concentration of most cannabinoids in female flowers are two-fold higher than the concentration in the inflorescence leaves (Bernstein et al. 2019b). In this study, flower tissue showed the highest cannabinoid production among three tissues. In flowers, the production of CBDA and THCA appeared to be the most predominant, producing 11,848 μg/g (1.1% w/w) and 12,028 μg/g (1.2% w/w), respectively (Supplementary Fig. 1). The floral production of CBDA were 2.4-fold higher than the production in leaf tissues (n = 24, p < 0.0001) and 25-fold higher than the production in stem tissues (n = 24, p < 0.0001) (Supplementary Fig. 1). Similarly, the production of THCA was 2.3-fold higher production than the production in leaf tissues (n = 24, p < 0.0001) and 29.8% higher than the production in stem tissues (n = 24, p < 0.0001) (Supplementary Fig. 1). Other cannabinoids including CBGA, CBG, CBD, and THC were produced less than 0.05%. However, the levels were consistently high in flower tissues than leaf and stem tissues (Supplementary Fig. 1).
Floral cannabinoid production on day 7, 12, and 14 after the transition to the short-day were measured using HPLC. The cannabinoid analyses showed that the amount of CBDA increased 1.5-fold from 11,848 μg/g (1.1% w/w) at day 7 to 18,204 μg/g (1.8% w/w) at day 14 (Supplementary Fig. 2C). The level of total CBD increased 1.6-fold from 11,090 μg/g (1.1% w/w) at day 7 to 17,705 μg/g (1.7% w/w) at day 14 (Supplementary Fig. 2G). Additionally, the levels of CBD and THC increased 2.5-fold (699 μg/g; 0.06% w/w to 1740 μg/g; 0.1% w/w) and 4-fold (1,089 μg/g; 0.1% w/w to 4320 μg/g; 0.4% w/w), respectively (Supplementary Fig. 2D, F). However, other cannabinoids such as CBGA, CBG, THCA, and total THC remained unchanged during the first 2 weeks of flowering (Supplementary Fig. 2A, B, E, and H).
Leaf cannabinoids were also measured at the same time regime. The production of CBDA and THCA were 4868 μg/g (0.48% w/w) and 5220 μg/g (0.52% w/w), respectively at day 7. However, the concentrations did not change during the early flowering stage (Supplementary Fig. 2A–F).
These results suggest selective activation of flower cannabinoids biosynthetic genes. By deactivating the cannabinoid production in other tissues, presumably the catalytic energy and carbons used in leaf tissues were redirected to the flower organ for concentrating cannabinoid production in the specialized trichome cells. Supplementary Table 1 presents the measured floral cannabinoid concentrations of the immature flower tissues from control plants (day 1) and stress-treated plant (day 6 or day 8) that were used to calculate the production values during that timeframe.
These results are consistent with the previous studies that most cannabinoids production is organ and location–specific, with the trichome-dense flowers being the organs that produce the greatest amount of cannabinoids (Bernstein et al. 2019b). Another study also showed that cannabinoid production can vary greatly among different inflorescence locations with greater concentrations toward the apical meristem (Namdar et al. 2018).
Cannabinoid productions in response to mechanical wounds
Field-grown Cannabis is constantly exposed to adverse biotic (e.g., microbial and herbivore pests), abiotic (e.g., excess heat, drought, and wind), and man-made stresses (e.g., tractor). These stresses have been reported to significantly impact cannabinoid production.
To investigate how mechanical damage affects cannabinoid metabolism, hemp clones (7 weeks old) were tested in grow tents located in a greenhouse. Treatments were started during the first week of flower to elucidate the greatest recordable amount of response, and to avoid the senescence phase of growth. Plants were harvested for the temporal- and spatial-specific cannabinoid analyses 14 days after the transition to the short-day, which limited this study to understanding the effects of these stresses on the onset of flowering; however, future studies should investigate the impact these stresses have on mature flower.
Figure 1 shows the changes of cannabinoid accumulation in three Cannabis tissues—immature flower, leaf, and stem—in response to mechanical wounding. The seven cannabinoid compounds described above were quantified using HPLC. The cannabinoid level observed after 5 days of treatment was compared to the 5-day chemical profile difference shown in the control plants. In the control plants, the cannabinoid production remained about the same level for 5 days. The mechanical wounding also did not impact the level of any cannabinoids (n = 3, p > 0.05) in any tissues of the plants (Fig. 1 and Table 1). In leaf and stem tissues, only CBDA and THCA were quantifiable and appeared not to be changed after mechanical wounding (n = 3, p > 0.05). Other cannabinoid compounds such as CBGA and CBG were under detectable limit in both treated and control plants.
| Mechanical wound (5-day) | Herbivore (5-day) | Excess heat (7-day) | Drought (7-day) | |||||
|---|---|---|---|---|---|---|---|---|
| Control (μg/g) | Treatment (μg/g) | Control (μg/g) | Treatment (μg/g) | Control (μg/g) | Treatment (μg/g) | Control (μg/g) | Treatment (μg/g) | |
| CBGA | − 130 ± 663 | 172 ± 424 | 308 ± 168 | − 24 ± 47** | 206 ± 147 | − 182 ± 133*** | 265 ± 103 | 34 ± 188 |
| CBG | − 2 ± 28 | 49 ± 51 | 69 ± 85 | − 52 ± 43* | 21 ± 29 | − 112 ± 105* | 336 ± 49 | 622 ± 110*** |
| CBDA | 611 ± 3216 | 7223 ± 4113 | 671 ± 2108 | − 1367 ± 1053 | − 1948 ± 3065 | − 3081 ± 1442 | 4131 ± 3065 | 826 ± 4417 |
| CBD | − 174 ± 354 | 249 ± 162 | 755 ± 397 | 194 ± 121* | − 55 ± 174 | − 338±471 | 1182 ± 60 | 297 ± 267**** |
| THCA | 593 ± 3596 | 7112 ± 3671 | 200 ± 2825 | − 806 ± 911 | − 1917 ± 2129 | − 2829±718 | 3201 ± 4801 | 3849 ± 3851 |
| THC | − 596 ± 734 | 232 ± 421 | 1771 ± 1034 | 687 ± 301 | − 21 ± 398 | − 1137 ± 1391 | 3927 ± 242 | 580 ± 555**** |
Several studies have revealed that short-term mechanical damage affects the production of secondary metabolites in cotton (Park et al. 2019b), Catharanthus roseus (Chen et al. 2018), sugar beet (Lafta and Fugate 2011), and lettuce (Saltveit 2000). These studies showed that the production of secondary metabolites (i.e., terpenoids, alkaloids, and phenolic compounds) that play an important role in direct defense were increased by the abiotic stress. Unlike these crops, short-term mechanical stress (1–5 days) did not affect the cannabinoid production in the studied hemp variety. While we did not study long-term effects of this mechanical damage, it appears that 5 days was not sufficient to induce any biosynthetic changes in the phytocannabinoid production. Future studies will be needed to understand the long-term effects on mature flower chemometrics; however, it does not appear to affect a hemps plant ability to produce cannabinoids at the onset of flower.
Cannabinoid productions in response to herbivore stress
Insect pests can be classified by how they infest Cannabis, such as insects with “chewing mouth parts” affect the roots, leaves, stems, and flowers, and “piercing-sucking” insects can bypass insecticidal cannabinoids on the surface of the plant to access the sap within the plant (McPartland 1996). The vast nature of the types of insects that affect Cannabis cultivation provides numerous outcomes when infested and activates various stress responses depending on the insect. Thus, this investigation of the cannabinoid content response to particular insects is essential to field-grown hemp since cannabinoids are one of the most valued products of the Cannabis plant.
To examine how the insect herbivores affect the cannabinoid production and composition, 20 3rd instar caterpillar larvae of tobacco hornworm Manduca sexta were placed on the 7-week-old hemp plants’ leaves for 5 days. It was observed that the larval insects preferentially feed on leaf tissues over stems, flowers, bracts, and petals. Figure 2 shows quantitative comparisons of 5 days of cannabinoid production between control and insect damaged hemp plants. The herbivore wounding significantly reduced the cannabinoid production of CBGA, with the control plants accumulating 308 μg/g (0.03% w/w) to the treated plants losing 24 μg/g (0.0024% w/w) (p < 0.01), CBG, accumulating 69 μg/g (0.0069% w/w) in control plants to losing 52 μg/g (0.0052% w/w) in treated plants (p < 0.05), and CBD, accumulating 755 μg/g (0.075% w/w) in control plants to accumulating 194 μg/g (0.019% w/w) in treated plants (p < 0.05) while other cannabinoids, CBDA, THCA, and THC levels (Fig. 2 and Table 1) remained unchanged during the 7-day observation window. While the reduction of CBGA, CBG and CBD are significant, the treatment procedure could be improved by replacing the porous screen with a non-light blocking insect containment; however, due to the minimal light interference (4.3% photosynthetically active radiation reduction) observed here, it suggests the changes that occurred were due solely to the insect pressure, although future studies should verify these results with differing insect contaminant approaches.
Manduca sexta caterpillar regurgitates onto the wounded site of a host plant while feeding (Paudel Timilsena and Mikó 2017). Insect regurgitant contains small molecular elicitors such as fatty acid conjugates, inceptin, and calliferins, as well as larger enzymatic molecules such as a glucose oxidase protein (Paudel Timilsena and Mikó 2017). The regurgitant is used to suppress plant defense mechanisms, leading to the changes in metabolic profiles that involve the release of toxic chemicals such as alkaloids, anthocyanins, phenols, and quinones, as well as volatile terpenoids that repel natural enemy insects (War et al. 2012). However, it was unexpected that the insect damage decreased cannabinoid production as they have been previously considered an effective stimulator to stress response (Benelli et al. 2018; Park et al. 2019a). The observed decrease is likely due to cannabinoid biosynthesis not being triggered by this particular herbivore’s stressors, the regurgitant suppressing the plant’s defense response, or the signal to increase production may not have been observable within the limited 5-day window of this study.
Cannabinoid production in response to excess heat
Hemp grows ideally at 24–30 °C in nitrogen-enriched fertilized soils (pH 6.0–7.5) under a regime of 16–24 h of light and 0–8 h of darkness with 40–60% humidity level (Adesina et al. 2020; Chandra et al. 2017). In fields, higher temperatures (> 31 °C) are a common stressor that alters plant physiology and metabolism. To examine how excess heat affects cannabinoid production, six hemp clones were heat-treated at 45–50 °C over 7 days and six clones served as controls at 22–27 °C. Figure 3 shows quantitative comparisons of cannabinoid production between control and heat-treated hemp plants over the 7-day period. Within 3 days, the hemp plants were completely wilted under excess heat regardless of the water supply ( 1L/day). It should be noted that plants were also exposed to water stress in addition to the heat stress due to the increased transpiration caused by the increased temperature. The HPLC demonstrated that excess heat caused significant cannabinoid metabolic changes. In the untreated control plants, female inflorescence produced 206 μg/g (0.02% w/w) of CBGA and 21 μg/g (0.0021% w/w) of CBG during the 7-day observation window. After 7 days of excessive heat treatment, the concentration of CBGA and CBG decreased by 182 μg/g (0.0182% w/w) (n = 3, p < 0.001 and p < 0.05) and by 112 μg/g (0.0112% w/w) (n = 3, p < 0.05), respectively (Fig. 3 and Table 1). Contrastingly, CBDA, THCA, CBD, and THC bioaccumulations were not changed during this 7-day window (Fig. 3 and Table 1).
As with all cannabinoids, it was expected to see an increase in concentration over the 7-day period; however, heat stress caused the opposite effect. With the decreased concentrations of CBGA and CBG, it would be hypothesized that the enzymatic conversion of CBGA to THCA and CBDA would be happening at a faster rate in the treated plants causing an increase of the terminal cannabinoid concentrations while depleting the precursor pool. However, no significant difference was observed in the concentrations of THCA and CBDA, thus it appears the enzymatic conversion was not affected and the biosynthesis of CBGA may have been downregulated or inhibited upstream in the cannabinoid biosynthetic pathway. While we cannot definitively say whether it was the heat stress or watering habits that affected this cannabinoid production, this result does provide support for a potential downregulation of CBGA production during the initiation of flowering, which would be hypothesized to decrease overall cannabinoid production if the study would have observed longer into the flowering stage.
Cannabinoid productions in response to drought
Figure 4 and Table 1 show the cannabinoid production in response to 7 days of drought stress in the various hemp tissues. Notably, the drought treatment has changed the biosynthesis of CBG, CBD, and THC. Unlike other stresses investigated, drought significantly increased CBG production by 40% while CBD and THC were dramatically reduced by 70–80%. The control plants accumulated 336 μg/g (0.03% w/w) of CBG during the 8-day window, whereas, the amount accumulated in the treated plants significantly increased to 622 μg/g (0.06% w/w) (n = 3, p < 0.001). In addition, two other downstream products, CBD and THC concentrations were significantly decreased from accumulating 1182 μg/g (0.12% w/w) of CBD in the control plants to only accumulating 296 μg/g (0.02% w/w) of CBD in the plants subjected to drought stress (n = 3, p < 0.0001). Similarly, the control plants produced 3927 μg/g (0.39% w/w) of THC during this 8-day period, whereas the plants subjected to drought only accumulated 580 μg/g (0.05% w/w) of THC (n = 3, p < 0.0001).
CBG is a shared precursor molecule to the production of both CBD and THC. The increase of CBG accumulation might indicate the blockage of conversion into the two downstream intermediates, CBDA and THCA, resulting in accumulation of CBGA that was decarboxylated to CBG under these stress conditions. The catalytic enzymes, CBDA and THCA synthases may have malfunctioned enzymatically and/or their genes’ expression was downregulated resulting in less enzyme available. The reduced enzymatic activity consequently resulted in the decrease of downstream end-products (CBD and THC) while the precursor CBG levels accumulate. Water deficit is directly related to a variety of cellular processes including carbohydrate transport and metabolism, signal transduction mechanisms, and secondary metabolite biosynthesis, transport, and catabolism (Gao et al. 2018). Similar to their findings, in this study, drought stress resulted in the decreased levels of end-product cannabinoids.
Additional work should investigate if drought also affects other secondary metabolites such as terpenoids by measuring terpenoid content in response to drought stress, as well as time-specific drought stresses throughout the flower stage to determine the overall effects on cannabinoid concentration.
Conclusion
Cannabinoid analyses supported previous studies that floral cannabinoid production is at least 2.5-fold greater than in the leaf tissues. Cannabinoid production at the onset of flowering is negatively associated with herbivory, excess heat, and drought while mechanical wounding showed no impact. These common field stresses are adequate to trigger changes in the cannabinoid profiles at the early flowering stage, especially drought which is the most impactful restraint for hemp growth in terms of cannabinoid production (70–80% reduction in CBD and THC). Further studies are necessary to validate if the observed changes apply to mature buds and understand the hypothesized underlying gene regulation causing these increases or decreases in cannabinoid concentrations. This study provides an initial understanding of the effects of biotic and abiotic stresses common when initiating flowering in hemp, as well as providing an understanding of the stresses that are most impactful to the onset of flowering to guide future studies to determine these various stresses’ effects, if they exists, on the chemical profile of mature hemp flowers.
Supplementary Information
Untitled section
Acknowledgements
Not applicable.
Abbreviations
- CBGA
- Cannabigerolic acid
- CBG
- Cannabigerol
- CBDA
- Cannabidiolic acid
- CBD
- Cannabidiol
- THCA
- Δ-Tetrahydrocannabinolic acid
- THC
- Δ-Tetrahydrocannabinol
- CBN
- Cannabinol
Funding
This study was funded by the Institute of Cannabis Research (ICR).
Availability of data and materials
All data generated or analyzed in this study are included in this published article.
Declarations
Ethics approval and consent to participate
Not applicable.
Consent for publication
All the authors consent to publish this study at the Journal of Cannabis Research.
Competing interests
The authors declare that they have no competing interests.
Footnotes
Footnote Group
References
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References
- Adesina I, Bhowmik A, Sharma H, Shahbazi A. A review on the current state of knowledge of growing conditions, agronomic soil health practices and utilities of hemp in the United States. Agriculture. 2020;10(4):129. doi: 10.3390/agriculture10040129.
- Aubin M-P, Seguin P, Vanasse A, Lalonde O, Tremblay GF, Mustafa AF, et al. Evaluation of eleven industrial hemp cultivars grown in eastern Canada. Agron J. 2016;108(5):1972–1980. doi: 10.2134/agronj2016.04.0217.
- Backer R, Schwinghamer T, Rosenbaum P, McCarty V, Eichhorn Bilodeau S, Lyu D, et al. Closing the yield gap for Cannabis: a meta-analysis of factors determining Cannabis yield. Front Plant Sci. 2019;10:495. doi: 10.3389/fpls.2019.00495.
- Benelli G, Pavela R, Petrelli R, Cappellacci L, Santini G, Fiorini D, et al. The essential oil from industrial hemp (Cannabis sativa L.) by-products as an effective tool for insect pest management in organic crops. Ind Crops Prod. 2018;122:308–315. doi: 10.1016/j.indcrop.2018.05.032.
- Bernstein N, Gorelick J, Zerahia R, Koch S. Impact of N, P, K, and humic acid supplementation on the chemical profile of medical Cannabis (Cannabis sativa L). Front Plant Sci. 2019a;10(736). 10.3389/fpls.2019.00736.
- Bernstein N, Gorelick J, Koch S. Interplay between chemistry and morphology in medical cannabis (Cannabis sativa L.). Ind Crops Prod. 2019b;129:185–94. 10.1016/j.indcrop.2018.11.039.
- Burgel L, Hartung J, Schibano D, Graeff-Honninger S. Impact of different phytohormones on morphology, yield and cannabinoid content of Cannabis sativa L. Plants (Basel) 2020;9(6):725. doi: 10.3390/plants9060725.
- Campbell BJ, Berrada AF, Hudalla C, Amaducci S, McKay JK. Genotype × environment interactions of industrial hemp cultivars highlight diverse responses to environmental factors. Agrosyst Geosci Environ. 2019;2(1):180057. doi: 10.2134/age2018.11.0057.
- Caplan D, Dixon M, Zheng Y. Increasing inflorescence dry weight and cannabinoid content in medical Cannabis using controlled drought stress. HortScience. 2019;54(5):6. doi: 10.21273/HORTSCI13510-18.
- Chandra S, Lata H, ElSohly AM. Cannabis sativa L. - botany and biotechnology. Cham: Springer; 2017.
- Chandra S, Lata H, Khan IA, ElSohly MA. The role of biotechnology in Cannabis sativa propagation for the production of phytocannabinoids. Berlin: Springer Berlin Heidelberg; 2013. p. 123–48.
- Chen Q, Lu X, Guo X, Liu J, Liu Y, Guo Q, et al. The specific responses to mechanical wound in leaves and roots of Catharanthus roseus seedlings by metabolomics. J Plant Interact. 2018;13(1):450–460. doi: 10.1080/17429145.2018.1499970.
- Citterio S, Prato N, Fumagalli P, Aina R, Massa N, Santagostino A, et al. The arbuscular mycorrhizal fungus Glomus mosseae induces growth and metal accumulation changes in Cannabis sativa L. Chemosphere. 2005;59(1):21–29. doi: 10.1016/j.chemosphere.2004.10.009.
- Dambolena JS, Zunino MP, Herrera JM, Pizzolitto RP, Areco VA, Zygadlo JA. Terpenes: natural products for controlling insects of importance to human health—a structure-activity relationship study. Psyche. 2016;2016:4595823. doi: 10.1155/2016/4595823.
- Danziger N, Bernstein N. Light matters: effect of light spectra on cannabinoid profile and plant development of medical cannabis (Cannabis sativa L.) Ind Crops Prod. 2021;164:113351. doi: 10.1016/j.indcrop.2021.113351.
- Danziger N, Bernstein N. Plant architecture manipulation increases cannabinoid standardization in ‘drug-type’ medical cannabis. Ind Crops Prod. 2021;167:113528. doi: 10.1016/j.indcrop.2021.113528.
- de Meijer EPM, Hammond KM. The inheritance of chemical phenotype in Cannabis sativa L. (II): Cannabigerol predominant plants. Euphytica. 2005;145(1):189–198. doi: 10.1007/s10681-005-1164-8.
- de Meijer EPM, Hammond KM, Micheler M. The inheritance of chemical phenotype in Cannabis sativa L. (III): variation in cannabichromene proportion. Euphytica. 2009;165(2):293–311. doi: 10.1007/s10681-008-9787-1.
- de Meijer EPM, Hammond KM, Sutton A. The inheritance of chemical phenotype in Cannabis sativa L. (IV): cannabinoid-free plants. Euphytica. 2009;168(1):95–112. doi: 10.1007/s10681-009-9894-7.
- Ebersbach P, Stehle F, Kayser O, Freier E. Chemical fingerprinting of single glandular trichomes of Cannabis sativa by Coherent anti-Stokes Raman scattering (CARS) microscopy. BMC Plant Biol. 2018;18(1):275. doi: 10.1186/s12870-018-1481-4.
- Egamberdieva D, Wirth SJ, Alqarawi AA, Abd Allah EF, Hashem A. Phytohormones and beneficial microbes: essential components for plants to balance stress and fitness. Front Microbiol. 2017;8:2104. doi: 10.3389/fmicb.2017.02104.
- Eichhorn Bilodeau S, Wu BS, Rufyikiri AS, MacPherson S, Lefsrud M. An update on plant photobiology and implications for Cannabis production. Front Plant Sci. 2019;10:296. doi: 10.3389/fpls.2019.00296.
- Elsohly MA, Slade D. Chemical constituents of marijuana: the complex mixture of natural cannabinoids. Life Sci. 2005;78(5):539–548. doi: 10.1016/j.lfs.2005.09.011.
- Flores-Sanchez IJ, Pec J, Fei J, Choi YH, Dusek J, Verpoorte R. Elicitation studies in cell suspension cultures of Cannabis sativa L. J Biotechnol. 2009;143(2):157–168. doi: 10.1016/j.jbiotec.2009.05.006.
- Fu ZQ, Dong X. Systemic acquired resistance: turning local infection into global defense. Annu Rev Plant Biol. 2013;64:839–863. doi: 10.1146/annurev-arplant-042811-105606.
- Gao C, Cheng C, Zhao L, Yu Y, Tang Q, Xin P, et al. Genome-wide expression profiles of hemp (Cannabis sativa L.) in response to drought stress. Int J Genomics. 2018;2018:3057272. doi: 10.1155/2018/3057272.
- García-Tejero IF, Durán Zuazo VH, Sánchez-Carnenero C, Hernández A, Ferreiro-Vera C, Casano S. Seeking suitable agronomical practices for industrial hemp (Cannabis sativa L.) cultivation for biomedical applications. Ind Crops Prod. 2019;139:111524. doi: 10.1016/j.indcrop.2019.111524.
- Gonçalves J, Rosado T, Soares S, Simão AY, Caramelo D, Luís Â, et al. Cannabis and its secondary metabolites: their use as therapeutic drugs, toxicological aspects, and analytical determination. Medicines (Basel) 2019;6(1):31. doi: 10.3390/medicines6010031.
- Gorelick J, Bernstein N. Cannabis sativa L.: botany and horticulture. In: Chandra S, Lata H, ElSohly MA, editors. Cannabis sativa L: - botany and biotechnology. Cham: Springer International Publishing; 2017. pp. 444–461.
- Herppich WB, Gusovius H-J, Flemming I, Drastig K. Effects of drought and heat on photosynthetic performance, water use and yield of two selected fiber hemp cultivars at a poor-soil site in Brandenburg (Germany) Agronomy. 2020;10(9):1361. doi: 10.3390/agronomy10091361.
- Husain R, Weeden H, Bogush D, Deguchi M, Soliman M, Potlakayala S, et al. Enhanced tolerance of industrial hemp (Cannabis sativa L.) plants on abandoned mine land soil leads to overexpression of cannabinoids. PLoS One. 2019;14(8):e0221570. doi: 10.1371/journal.pone.0221570.
- Kim E-S, Mahlberg PG. Immunochemical localization of tetrahydrocannabinol (THC) in cryofixed glandular trichomes of Cannabis (Cannabaceae) Am J Bot. 1997;84(3):336–342. doi: 10.2307/2446007.
- Kovalchuk O, Li D, Rodriguez-Juarez R, Golubov A, Hudson D, Kovalchuk I. The effect of cannabis dry flower irradiation on the level of cannabinoids, terpenes and anti-cancer properties of the extracts. Biocatal Agric Biotechnol. 2020;29:101736. doi: 10.1016/j.bcab.2020.101736.
- Lafta AM, Fugate KK. Metabolic profile of wound-induced changes in primary carbon metabolism in sugarbeet root. Phytochemistry. 2011;72(6):476–489. doi: 10.1016/j.phytochem.2010.12.016.
- Lalge AB, Mendel P, Vyhnanek T, Trojan V, Kalousek P, Havel L. Effects of different morphoregulators on growth and development of Cannabis sativa L. In: Proceedings of the International PhD Students Conference on MendelNet 2016, vol. 2016. Czech Republic: MendelNet 2016; 2016. p. 726–30.
- Langenheim JH. Higher plant terpenoids: a phytocentric overview of their ecological roles. J Chem Ecol. 1994;20(6):1223–1280. doi: 10.1007/BF02059809.
- Leon J, Rojo E, Sanchez-Serrano JJ. Wound signalling in plants. J Exp Bot. 2001;52(354):1–9. doi: 10.1093/jexbot/52.354.1.
- Linger P, Ostwald A, Haensler J. Cannabis sativa L. growing on heavy metal contaminated soil: growth, cadmium uptake and photosynthesis. Biol Plant. 2005;49(4):567–576. doi: 10.1007/s10535-005-0051-4.
- Livingston SJ, Quilichini TD, Booth JK, Wong DCJ, Rensing KH, Laflamme-Yonkman J, et al. Cannabis glandular trichomes alter morphology and metabolite content during flower maturation. Plant J. 2020;101(1):37–56. doi: 10.1111/tpj.14516.
- Luo X, Reiter MA, d’Espaux L, Wong J, Denby CM, Lechner A, et al. Complete biosynthesis of cannabinoids and their unnatural analogues in yeast. Nature. 2019;567(7746):123–126. doi: 10.1038/s41586-019-0978-9.
- Magagnini G, Grassi G, Kotiranta S. The effect of light spectrum on the morphology and cannabinoid content of Cannabis sativa L. Med Cannabis Cannabinoids. 2018;1(1):19–27. doi: 10.1159/000489030.
- Mansouri H, Asrar Z. Effects of abscisic acid on content and biosynthesis of terpenoids in Cannabis sativa at vegetative stage. Biol Plant. 2012;56(1):153–156. doi: 10.1007/s10535-012-0033-2.
- Mansouri H, Asrar Z, Szopa J. Effects of ABA on primary terpenoids and Δ9-tetrahydrocannabinol in Cannabis sativa L. at flowering stage. Plant Growth Regul. 2009;58(3):269–277. doi: 10.1007/s10725-009-9375-y.
- McPartland JM. Cannabis pests. J Int Hemp Assoc. 1996;3(2):4.
- McPartland JM. Epidemiology of the hemp borer, Grapholita delineanaWalker (Lepidoptera: Oleuthreutidae), a pest of Cannabis sativa L. J Ind Hemp. 2002;7(1):25–42. doi: 10.1300/J237v07n01_04.
- McPartland JM, Clarke RC, Watson DP. Hemp diseases and pests: management and biological control. Oxfordshire: CABI Publishing; 2000.
- Mittler R, Blumwald E. The roles of ROS and ABA in systemic acquired acclimation. Plant Cell. 2015;27(1):64–70. doi: 10.1105/tpc.114.133090.
- Montoya Z, Conroy M, Vanden Heuvel BD, Pauli CS, Park S-H. Cannabis contaminants limit pharmacological use of cannabidiol. Front Pharmacol. 2020;11(1439). 10.3389/fphar.2020.571832.
- Namdar D, Mazuz M, Ion A, Koltai H. Variation in the compositions of cannabinoid and terpenoids in Cannabis sativa derived from inflorescence position along the stem and extraction methods. Ind Crops Prod. 2018;113:376–382. doi: 10.1016/j.indcrop.2018.01.060.
- Pagnani G, Pellegrini M, Galieni A, D’Egidio S, Matteucci F, Ricci A, et al. Plant growth-promoting rhizobacteria (PGPR) in Cannabis sativa ‘Finola’ cultivation: an alternative fertilization strategy to improve plant growth and quality characteristics. Ind Crops Prod. 2018;123:75–83. doi: 10.1016/j.indcrop.2018.06.033.
- Park SH, Scheffler J, Scheffler B, Cantrell CL, Pauli CS. Chemical defense responses of upland cotton, Gossypium hirsutum L. to physical wounding. Plant Direct. 2019;3(5):e00141. doi: 10.1002/pld3.141.
- Park SH, Staples SK, Gostin EL, Smith JP, Vigil JJ, Seifried D, et al. Contrasting roles of cannabidiol as an insecticide and rescuing agent for ethanol-induced death in the tobacco hornworm Manduca sexta. Sci Rep. 2019;9(1):10481. doi: 10.1038/s41598-019-47017-7.
- Paudel Timilsena B, Mikó I. Know your insect: the structural backgrounds of regurgitation, a case study on Manduca sexta and Heliothis virescens (Lepidoptera: Sphingidae, Noctuidae) Res Ideas Outcomes. 2017;3:e11997. doi: 10.3897/rio.3.e11997.
- Pauli CS, Conroy M, Vanden Heuvel BD, Park SH. Cannabidiol drugs clinical trial outcomes and adverse effects. Front Pharmacol. 2020;11:63. doi: 10.3389/fphar.2020.00063.
- Peč J, Flores-Sanchez IJ, Choi YH, Verpoorte R. Metabolic analysis of elicited cell suspension cultures of Cannabis sativa L. by 1H-NMR spectroscopy. Biotechnol Lett. 2010;32(7):935–941. doi: 10.1007/s10529-010-0225-9.
- Ramakrishna A, Ravishankar GA. Influence of abiotic stress signals on secondary metabolites in plants. Plant Signal Behav. 2011;6(11):1720–1731. doi: 10.4161/psb.6.11.17613.
- Saloner A, Bernstein N. Response of medical Cannabis (Cannabis sativa L.) to nitrogen supply under long photoperiod. Front Plant Sci. 2020;11(1517). 10.3389/fpls.2020.572293.
- Saltveit ME. Wound induced changes in phenolic metabolism and tissue browning are altered by heat shock. Postharvest Biol Technol. 2000;21(1):61–69. doi: 10.1016/S0925-5214(00)00165-4.
- Savatin DV, Gramegna G, Modesti V, Cervone F. Wounding in the plant tissue: the defense of a dangerous passage. Front Plant Sci. 2014;5:470. doi: 10.3389/fpls.2014.00470.
- Shipony S, Bernstein N. The highs and lows of P supply in medical cannabis: effects on cannabinoids, the ionome and morpho-physiology. Front Plant Sci. 2021. 10.3389/fpls.2021.657323.
- Sirikantaramas S, Taura F, Tanaka Y, Ishikawa Y, Morimoto S, Shoyama Y. Tetrahydrocannabinolic acid synthase, the enzyme controlling marijuana psychoactivity, is secreted into the storage cavity of the glandular trichomes. Plant Cell Physiol. 2005;46(9):1578–1582. doi: 10.1093/pcp/pci166.
- Small E, Marcus D, Butler G, McElroy AR. Apparent increase in biomass and seed productivity in hemp (Cannabis sativa) resulting from branch proliferation caused by the European corn borer (Ostrinia nubilalis) J Ind Hemp. 2007;12(1):15–26. doi: 10.1300/J237v12n01_03.
- UNODC . Crime UNOoDa. United Nations: United Nations Office on Drugs and Crime; 2009. Recommended methods for the identification and analysis of Cannabis and Cannabis products.
- Van Der Werf HMG, Brouwer K, Wijlhuizen M, Withagen JCM. The effect of temperature on leaf appearance and canopy establishment in fibre hemp (Cannabis sativa L.) Ann Appl Biol. 1995;126(3):551–561. doi: 10.1111/j.1744-7348.1995.tb05389.x.
- Wang M, Wang YH, Avula B, Radwan MM, Wanas AS, van Antwerp J, et al. Decarboxylation study of acidic cannabinoids: a novel approach using ultra-high-performance supercritical fluid chromatography/photodiode array-mass spectrometry. Cannabis Cannabinoid Res. 2016;1(1):262–271. doi: 10.1089/can.2016.0020.
- War AR, Paulraj MG, Ahmad T, Buhroo AA, Hussain B, Ignacimuthu S, et al. Mechanisms of plant defense against insect herbivores. Plant Signal Behav. 2012;7(10):1306–1320. doi: 10.4161/psb.21663.
- White KH, Vergara D, Keepers KG, Kane NC. The complete mitochondrial genome for Cannabis sativa. Mitochondrial DNA B Resour. 2016;1(1):715–716. doi: 10.1080/23802359.2016.1155083.
- Williamson EM. wi.: London. Pages: 448. ISBN: 0-85369-517-2. London: EPharmaceutical Press; 2004.
- Winston ME, Hampton-Marcell J, Zarraonaindia I, Owens SM, Moreau CS, Gilbert JA, et al. Understanding cultivar-specificity and soil determinants of the cannabis microbiome. PLoS One. 2014;9(6):e99641. doi: 10.1371/journal.pone.0099641.
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Data Availability Statement
All data generated or analyzed in this study are included in this published article.