Effects of 5-Aminolevulinic Acid (ALA) on Zinnia hybrida Growth and Phytoremediation Effects in Oil-Contaminated Soil ()
1. Introduction
Petroleum is an essential substance and is used as fuel or lubricant for a variety of purposes. The broad application of petroleum, however, leads to soil and ground water contamination in many places. Unfortunately, this wide-spread contamination has received limited research to date [1]. Oil-contamination of soil and groundwater negatively impacts human and environmental health [2], land deals, and other economic processes [3] [4]. Therefore, the Ministry of the Environment in Japan issued countermeasure guidelines and legal regulations on soil contamination by petroleum [5].
5-Aminolevulinic acid (ALA) is a key precursor in the biosynthesis of porphyrins, such as chlorophyll and heme, and may aid in the bioremediation of such contamination. The formation of ALA limits the rate of porphyrin biosynthesis [6] [7], as ALA levels concentrations are very low in vivo [8] [9]. In plants, ALA is synthesized from glutamate and appears to be highly regulated; this reaction requires a glutamyl-tRNA intermediate as well as ATP and NADPH cofactors [6] [7]. In enzyme preparations from Chlorella vulgaris [9] and higher plants [8], this step is inhibited by heme when supplied in the micromolar concentration range.
When treated with relatively higher concentrations, ALA has clear herbicidal properties. High ALA concentrations lead to the accumulation of several chlorophyll intermediates, such as protochlorophyllide and protoporphyrin IX [6] [10] [11] [12]. Most studies focusing on the physiological effects and herbicidal properties of ALA used higher concentrations (i.e. 5 - 40 mM) than what is found in vivo [13] [14] [15] [16] [17]. However, ALA stimulates plant growth at relatively lower concentrations [18] - [24]. Hotta et al. (1997b) [25] reported that foliar applications of 6 mM ALA damaged radish leaves, whereas applications of <1.8 mM increased radish growth and left the leaves undamaged. When using 0.1 - 1 ppm ALA for root applications, 30 - 100 ppm in foliar sprays, and 10 - 100 g/10 in soil treatments. Hotta et al. (1997a) [18] found that rice, corn, kidney bean, and radish seedlings grew an additional 10% - 50%.
The growth benefits of ALA may be due to its stimulation of photosynthesis [26] [27] [28]. Low ALA concentrations (i.e. 0.18 - 0.6 mM) have a variety of beneficial physiological effects to plants, including improved chlorophyll synthesis, photosynthetic activity, growth rates, respiration efficiency, and growth regulation [25] [29].
In terms of bioremediation, the degree of which oil-contaminated soils can be purified by plants (i.e. phytoremediation) is dependent on root growth. Kaimi et al. (2006) [30] reported that the rate of total petroleum hydrocarbon (TPH) reduction is greatest when root growth is most active and decreases as root growth slows. Kaimi et al. (2006) [30] and their team further suggested that root growth contributes to TPH degradation through the stimulation of microbial activity in the oil-contaminated soil.
The increased rates of photosynthesis and growth in ALA-treated plants would promote root growth, potentially stimulating microbial activity and TPH degradation in contaminated soil. Therefore, this study aims to discern the effect that ALA has on the growth and phytoremediation efficiency of Zinnia hybrida in oil-contaminated soil.
2. Materials and Methods
2.1. Preparation of Plant and Contaminated Soil
We previously studied 33 species of ornamental flowers and found that Zinnia hybrida exhibited the greatest phytoremediation capability within oil-contaminated soil [31]. Seeds of the Z. hybrida cultivar “Profusion White” were purchased from Sakata Seed Corporation (Yokohama, Japan). This greenhouse experiment was conducted at Meiji University’s experimental farm for 18 w.
We used commercial black soil. This type of soil, which has low air permeability and drainage but high water and fertilizer retention, is highly versatile and widely distributed throughout Japan. In a greenhouse, the soil was air dried for 3 w (until its moisture content was below 1% [w/w]), passed through 2 mm sieves, and stirred. Diesel oil was added uniformly with a pump sprayer. Contaminated soil was stirred once every 2 d for 14 d. The remaining oil particles were volatilised to prevent the negative effects of low molecular weight hydrocarbons on early plant growth [32]. For testing Z. hybrida’s remediation capability, we used an oil concentration of 4% by weight. The initial soil TPH concentration following volatilization was 9040 mg diesel kg−1 soil.
2.2. ALA Fertilizer Treatments
Similar to methods described by Mori and Chino (2018) [24], we treated soil with four different concentrations of ALA-based liquid fertilizer: 1500-fold (1500 plot), 5000-fold (5000 plot), and 8000-fold (8000 plot) dilutions, along with a non-treatment control (N plot). Soil (3 L) was placed in each 1/5000a Wagner pot. A commercial delayed release fertilizer (6% N, 40% P2O5, 6% K2O, 15% Mg; Company, Location) was mixed into the soil at a rate of 8 g∙L−1. Eight seeds were planted for each treatment and, after germination, thinned to two plants per pot. All pots were irrigated with 300 mL of water every 1 - 2 d, keeping the soil surface moist and avoiding run-off. Once per week, 300 mL of 500-fold diluted fertiliser (6% N, 10% P2O5, 5% K2O; Company, Location) was applied instead of water. Following 60 d after seedling, when ~8 leaves developed, ALA-based liquid fertilizer (Penta keep-V, Seiwa, Co., Ltd., Tochigi, Japan) was sprayed until shoots were moist; water was used on the control.
2.3. Plant Measurements
After 18 w, plants were harvested and analyzed for height, shoot fresh weight, shoot and root dry weight, soil dehydrogenase activity (DHA), and soil TPH concentration. At harvest, four pots per treatment were used for plant measurements. We measured the heights of the two plants in each pot, giving 8 plant height measurements per treatment. Roots were carefully washed. All the shoots and roots were harvested from each pot and the roots were washed carefully. The total dry weights of shoots and roots in each pot were measured after oven and plant matter was dried at 80˚C for 3 d; fresh and total dry weights of shoots and roots were measured per pot.
2.4. Analysis of Total Petroleum Hydrocarbon (TPH) Concentrations
Soil TPH concentrations were measured using guidelines from the Ministry of the Environment of Japan [5]; for details, see Ozawa et al. [31]. Plant roots were removed prior to analysis, which was repeated in triplicate for each sample. A gas chromatograph-hydrogen ionization detector (GC-FID, GC-2010, Shimadzu Corporation) was used to measure soil TPH concentrations. The soil in each pot was stirred and about 30 g was collected. For the extraction of TPH from the soil, the soil was dried in a 30˚C incubator (IN802, Yamato Kagaku Co., Ltd.) for 4 days to dehydrate the soil, 5 g was weighed in a 50 mL triangular flask, 15 mL of carbon disulfide (Wako Pure Chemical Industries, Ltd.) was added and extracted with shaking for 30 minutes, and the supernatant was allowed to stand for 2 hours. After the second and subsequent times, the incubation time was set at 1 h and the procedure was repeated three times, the extracted solution was scalped up to 50 mL. Unlike the method presented in the Guidelines for Oil Pollution Control (Ministry of the Environment, 2006), incubators were used for soil dewatering rather than anhydrous sodium sulfate, and extraction was performed three times before scale-up. The reasons for this are that light oil does not volatilize even after drying in the furnace, and we thought that three extractions might improve the extraction efficiency. The filtrate was filtered through a 0.45 µm pore size membrane filter (Millex® LH0.45 µm, Merck Ltd.) and the filtrate was injected into the GC-FID. The carrier gas was helium, and 1 µL of the sample extracted from the soil was injected in a splitless manner. Sample preparation and injection were performed using an auto-injector (AOC-20i, Shimadzu Corporation), and two replicates of analysis were performed per sample. The temperature program was held at 35˚C for 5 min and then raised to 320˚C at 10˚C/min. The column is a capillary column (Intercap 1MS, GL Science) with a liquid phase of 5% phenylmethyl silicon, 30 m long, 0.32 mm inside diameter, and 0.25 µm thickness.
2.5. Analysis of Soil Dehydrogenase Activity (DHA)
Plant roots were removed prior to analysis. Soil DHA levels were determined using the method of Hayase (1992) [33], modified as previously described in Ozawa et al. (2015) [31]. First, the soil in each pot was stirred and about 30 g was collected. 1 mL of 0.25 M Tris buffer (Sigma Aldrich) prepared with hydrochloric acid (Kokusan Chemical Co., Ltd.) at pH 6.8 to 1 g of soil and 0.4% 2-(4-iodophenyl)-3-(4-nitrophenyl)5-phenyltetrazolium chloride (INT) (Wako Pure Chemical Industries, Ltd.).) and 50 μL of 1% glucose (Wako Pure Chemical Industries, Ltd.) were added to a 100-mL test tube, sealed with plastic wrap, and incubated for 24 hours at 30˚C in the dark. Then, 10 mL of methanol (Wako Pure Chemical Industries, Inc.) was added to stop the enzymatic reaction, and the enzyme reaction was stopped, stirred in a vortex mixer (Titec Corporation) for 1 minute, and left to stand still for approximately 10 minutes, and the supernatant was filtered. Approximately 4 mL of filtrate was measured at 485 nm using a spectrophotometer (UV-1700, Shimadzu Corporation) to analyse the change from INT to iodonitrotetrazolium formazan (INTF), which has a high reduction activity. For the control area, the contaminated soil was sterilized by autoclave and then treated.
2.6. Statistical Analyses
Data are presented as means ± Standard deviation (SD). All data, except plant height (n = 8), were analysed at the pot level (n = 4) using a one-way analysis of variance and Fisher’s least significant difference (LSD) test. The data were analysed using Excel Statistics 2012 (Social Survey Research Information Co., Ltd., Tokyo, Japan) and an α of 0.05.
3. Results
3.1. Chemical and Biological Properties of Black Soil
Chemical properties of black soil are shown in Table 1. The TC, TN, TP, TK content values of the black soil were 59,520, 2692, 677, and 1106 mg∙kg−1, respectively. C/N ratio value of the black soil was 22.1. Furthermore, NO−3-N, NH+4-N, SP, and SK values of the black soil were 9.0, 0, 12.0, and 57.0 mg∙kg−1, respectively. In addition, pH was 5.5. EC was 0.14 mS cm−1.
Biological properties of black soil are shown in Table 2. Bacterial biomass number value was not detected. NH+4-N and NO-2-N oxidation activity values were 7.0, and 27.0, respectively. N and P circulation activity values were 1.0, and 0 points, respectively.
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Table 1. Chemical properties of black soil. zMean ± standard deviation of a sample (TC, TN, TP, TK, C/N ratio, NO−3-N, NH+4-N, SP, SK, pH, and EC: n = 4).
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Table 2. Biological properties of black soil. zMean ± standard deviation of a sample (bacterial biomass, NH+4-N oxidation activity, NO-2-N oxidation activity, N circulation activity, and P circulation activity: n = 4).
3.2. Comparison of Height, Weight of Zinnia hybrida
The plant heights, shoot fresh weights, and shoot and root dry weights after 18 w with N, 1500, 5000, and 8000 plots are shown in Table 3. Plant height values of N, 1500, 5000, and 8000 plots were 28.5, 32.2, 33.7, and 32.1 cm, respectively. Shoot fresh weight values of those plots were 17.07, 29.32, 35.84, and 27.77 g∙pot−1, respectively. Shoot dry weight values of those plots were 6.78, 7.18, 8.12, and 6.80 g∙pot−1, respectively. Root dry weight values of those plots were 1.28, 1.69, 2.45, and 1.37 g∙pot−1, respectively. ALA-treated plants were significantly taller than the control; however, there were no significant differences among ALA-treated plots. Root and shoot fresh and dry weights within the 5000 plot were significantly higher than the control 5000 plot and significantly lower at N plot.
3.3. Comparison of Soil TPH Concentrations and Soil DHA Levels
Soil TPH concentration and soil DHA level of N, 1500, 5000, and 8000 plots are shown in Table 4. Soil TPH concentration values of those plots were 6143.2, 4638.4, 3872.3, and 4819.2 mg∙kg−1-soil, respectively. Soil DHA level values of those plots were 9.31, 12.07, 13.86, and 11.85 mg INTF g−1 DW h−1, respectively. The DHA levels were higher at 5000 plot and lower at N pot (Table 4). In contrast, the TPH concentrations were significantly lower in 5000 plot and significantly higher within thin N plot (Table 4). This negative correlation between soil TPH and DHA levels is consistent with the literature [32].
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Table 3. Plant height (n = 8) and weights (n = 4) of Z. hybrida after 18 w of diluted ALA (plot) treatments.
*letters represent significantly different (p < 0.05) groups calculated using Fisher’s LSD.
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Table 4. Contaminated soil TPH concentrations and DHA levels (n = 4) after 18 w of Z. hybrida growth treated with different concentrations (plots) of ALA.
*letters represent significantly different (p < 0.05) groups calculated using Fisher’s LSD.
4. Discussion
Plant growth is enhanced at low concentrations (i.e. 30 - 100 ppm to 90 - 120 μmol∙L−1) of ALA treatments in a variety of plants [18] - [25] [29]. Several reports suggested that these stimulatory growth effects may be related to elevated chlorophyll synthesis, improved photosynthetic efficiency, increased net photosynthetic rate, and reduced respiration [20] [21] [25] [26] [27] [28] [29] [34] [35] ALA concentrations as little as 3 mM have even encouraged the accumulation of Chl b and LHC II apoproteins, stimulated chlorophyll and phycocyanin synthesis, and lead to increased growth [35] [36]. These reports are consistent with our findings, that ALA applications increase the growth of Z. hybrida.
The rhizosphere is an active environment that, through interactions among plants, microorganisms, and other organic substances, can break down contaminants, such as oil [37]. In fact, soil TPH decomposes more rapidly in the rhizosphere than in the non-rhizosphere [37] [38]. Root exudates, such as carboxylic acid, amino acid, protein, and sugars, may provide nutrients for microorganisms, enhancing microbial activity and increasing rhizosphere degradation activity. Root surfaces also become the location of growth for microorganisms because of abundant nutrients of the roots exudate, such as carboxylic acid, amino acid, protein, and sugars [32]. The rate of TPH degradation is greatest during the most active period of root growth and decreases when root growth declines [32] [39]. Our results support the idea that root growth increases the degree of purification in contaminated soils by oil.
ALA-treatments enhanced Z. hybrida photosynthesis activity and increased exudates from plant roots. These exudates may have provided nutrients for microorganisms and enhanced microbial activity in the oil-contaminated soil, resulting in the decreased TPH concentrations we observed. This effect was the highest at the 5000-fold diluted concentration, similar to the findings of Mori and Chino (2018) [24].
5. Conclusion
We sprayed ALA to the stems and leaves of Z. hybrida at different dilution concentrations of ALA: 1500-fold, 5000-fold, and 8000-fold dilutions, along with a non-treatment control of diluted ALA in oil-contaminated soil. The results showed that in plant growth, soil TPH was smaller and soil DHA level was larger when ALA was sprayed than when it was not sprayed. These results indicate that spraying ALA in combination with the growth of zinnia improves the purification effect of oil-contaminated soil. The best remediation effect was achieved by the 5000-FLOD dilution of ALA.