FT-IR study of the polysaccharides isolated from the skin juice, gel juice, and flower of Aloe vera tissues affected by fertilizer treatment
© Nejatzadeh-Barandozi and Enferadi; licensee Springer. 2012
Received: 15 April 2012
Accepted: 17 August 2012
Published: 24 October 2012
This experiment was conducted to evaluate the effect of different amounts of fertilizers on the polysaccharides of Aloe vera plant. There were four different treatments, viz. T1 = 150% N, T2 = 150% P, T3 = 150% K, and T4 = 150% NPK (50% N + 50% P + 50% K) soil. Crude water-soluble polysaccharides were isolated from the gel juice, skin juice, and flowers of A. vera planted in these soils.
Result indicates that skin juice contained 2.4 times the level of polysaccharides in gel juice from one plant, suggesting the potential industrial application of A. vera skin rather than discarding it. After anion-exchange chromatography, neutral polysaccharides accounted for 58.1% and 78.5% of the total recovered neutral and acidic polysaccharide preparations from the gel juice and skin juice, respectively, whereas the crude flower polysaccharides were largely composed of weakly acidic polysaccharides (84.2%). Sugar analysis of the polysaccharides after gel permeation chromatography revealed that glucose and galactose were the most abundant monosaccharide in the neutral polysaccharides from the gel juice and skin juice, respectively. The acidic polysaccharides from the two juices consisted of glucuronic acid, galactose, glucose, mannose, and xylose with variable proportions.
Except glucuronic acid (15.4%) in flower acidic polysaccharide, the flower neutral and acidic polysaccharides contained galactose, glucose, and mannose as the main sugar components. Glucuronic acid was the major uronic acid in all acidic polysaccharides from different tissues.
KeywordsAloe vera Polysaccharides Skin juice Gel juice Flower Fertilizer
Aloe vera (Liliaceae), one of the most widely cultivated species of the genus Aloe in the world, has been widely used for medicines and cosmetics, and its chemical constituents have been studied [1–4], different properties being ascribed to the inner, colorless leaf gel and to the exudate produced by the bundle sheath cells on the outer margin of the leaf. These major active ingredients, acting alone or in concert, include polysaccharides, glycoproteins, infiltrating exudate phenolics, and even, simplest of all, water. Polysaccharide fractions from water extracts of whole leaves of A. vera were found to lower blood glucose levels in normal mice and in alloxan-induced diabetic mice [5, 6].
Several workers have tried the separation of A. vera gel carbohydrate polymers into their polysaccharide components [5, 7, 8]. However, the types and molecular sizes of the polysaccharides extracted from aloe gel appear very diverse. The controversy of the previous reports may be due to plant subspecies or different geographical origin, seasonal and cultivar variation, technical differences used to isolate the polysaccharide, or degradation of polysaccharides by endogenous enzyme activity [9–11].
Now, the processing of A. vera gel, derived from the leaf pulp of the plant, has become a big industry worldwide due to its application in pharmaceutical and cosmetic industries. However, more and more aloe skin was discarded as waste. Very little is known about the bioactive substances in A. vera skin and the potential use of aloe skin in industry. The leaf skin preparation from A. vera was shown to lower blood glucose, and in artificially induced diabetic animals, normal insulin production was resumed . In yet another study, a carboxypeptidase was prepared from the ‘leaf skin’ and partially purified [3, 10, 13]. The compositional features of skin polysaccharides, alcohol insoluble complex, from other aloe species (A. vera) skin tissue have been studied . In addition, it has been reported that the flower of A. vera was rich in ascorbic acid [4, 14] and volatile components . To our knowledge, however, the isolation, purification, and compositional analysis of polysaccharides from the skin juice and flowers of A. vera effected by fertilizers have not been performed yet. In the present study, we report the fractionation and chemical composition of polysaccharides isolated from the skin juice and flowers of A. vera effected by fertilizers. The comparison of the chemical features of these polysaccharides with gel juice polysaccharides is also taken into consideration.
Plant material and tissue separation
This investigation was conducted at the National Institute of Genetic Engineering and Biotechnology (NIGEB), Tehran, Iran, during 2010. The climate of this area is subtropical. The soil of the experimental site was clay loam with a pH of 6.5. The experiment was laid out by randomized completely block design with four replications comprising four different treatments, viz. T1 = 150% N (100% N +50% P + 0% K), T2 = 150% P (50% N + 100% P + 0% K), T3 = 150% K (25% N + 25% P + 100% K), and T4 = 150% NPK (50% N + 50% P + 50% K) soil. Plants were grown in the greenhouse. Distance between the plants was 20 cm. Chemical fertilizers were used in this experiment as per treatment . A. vera plant and dried A. vera flower were available for this investigation. Fresh whole leaves, between 25 and 45 cm in length corresponding to 3-year-old plant, were washed, and the spikes, placed along their margins, were removed before slicing the leaf to separate the epidermis or skin from the filet. The skin and filet were washed extensively with distilled water to remove the exudates from their surfaces. Further, the skin and filet were cut into cubes, blended in a food processor (model HC380D, Tefal, Rumilly, France) at low speed, and squeezed through a 200-mesh screen. A. vera gel juice and skin juice were then centrifuged at 5,200×g (Universal Centrifuge DL-5, Shanghai, China) for 10 min to discard the callus. A. vera flower was initially dried at 70°C in an oven and ground using a food processor. These dried powders (100 g) were suspended in 500 ml of distilled water and refluxed for 2 h at 80°C. This extraction procedure was repeated three times, and the supernatants obtained were pooled and filtered on a Whatman no. 2 paper to remove the insoluble materials. Then, the clear supernatant was concentrated in a rotary evaporator under reduced pressure.
Extraction of crude polysaccharides from aloe skin juice, gel juice, and flower
The skin juice, gel juice, and the extracted flower solution, respectively, was mixed with four times volume of 95% (v/v) ethanol, stirred vigorously, and left overnight at 4°C. The precipitate was centrifuged at 5,200×g for 10 min, discarding the supernatant. The precipitate was redissolved in distilled water overnight and precipitated again by addition of four volumes of ethanol. The obtained precipitate was suspended in distilled water and treated with Sevag reagent (1-butanol:chloroform 1:4, v/v); after vigorous stirring on a vortex mixer for 10 min at room temperature and centrifugation at 5,200×g for 10 min, the supernatant solution was retreated in this manner until there was no free protein . Then, the flower polysaccharide solution was further treated with 2% activated charcoal to decolorize. The resulting solution was added with three volumes of 95% (v/v) ethanol to precipitate the polysaccharides. The crude polysaccharides were washed two times with absolute ethanol, acetone, and ethylether, and then completely dried at 40°C in an air oven for 48 h. The weights of the crude polysaccharides from the gel juice, skin juice, and flower were estimated respectively.
The crude polysaccharides were characterized using a Fourier transform infrared spectrophotometer (FT-IR; FTIR 8400S, Shimadzu, Tokyo, Japan). The dried polysaccharides were ground with KBr powder and pressed into pellets for FT-IR spectra measurement in the frequency range of 400 to 4,000 cm−1.
Purification of crude polysaccharides
The crude polysaccharides were separated by anion-exchange chromatography on a DEAE-Sephadex A-25 column (26 cm × 3 cm; GE Healthcare, Fairview, CT, USA). An amount of 50 mg of crude gel polysaccharide (CGP), crude skin polysaccharide (CSP), or crude flower polysaccharide (CFP) was dissolved in 10 ml of distilled water, filtered through a Millipore 0.45-μm filter (Millipore Co., Billerica, MA, USA), and applied onto the column at a flow rate of 1.2 ml/min. The neutral fraction was eluted with distilled water, while the weakly acidic fraction was eluted with 0.5 M NaCl, and then, the strongly acidic fraction was eluted with 1.0 M NaCl. Carbohydrates were detected in the 5-ml fractions by the phenol-H2SO4 method . The fractions with significant amount of carbohydrates were pooled, concentrated, dialyzed, and freeze-dried.
The freeze-dried polysaccharides were further purified, and the molecular weight distribution of the samples was measured by gel permeation chromatography on a Sepharose 4B column (42 cm × 2 cm, GE Healthcare). The column was calibrated with T-series dextrans of known molecular weights. The eluent was 0.1 M NaCl at a flow rate of 18 ml/h, and aliquots of 3 ml were collected. The fractions were assayed for carbohydrate as described above.
Chemical analysis of the polysaccharides
The total carbohydrate content was determined by the phenol-H2SO4 method , using glucose as the standard. Purified polysaccharide preparations (10 mg) were hydrolyzed with 2 M H2SO4 (5 ml, 100°C, 8 h) in a sealed ampoule under a nitrogen atmosphere , and the residual acid was neutralized with BaCO3 at 45°C. After centrifugation (5,200×g, 10 min), the supernatants were filtered through a Millipore 0.45-μm filter. The TLC analyses of hydrolysates were performed on silica gel 60 G (Merck, North Ryde, Australia) plates with n-propanol/water/pyridine (17:3:1, v/v) as the developing phase, and the neutral monosaccharide(s) and uronic acids in the hydrolysate were detected by spraying with diphenylamine/aniline/phosphoric acid (5:5:1, v/v), dried, and heated at 80°C for 15 min. Authentic monosaccharide standards were run along with the test samples.
The percentages of different neutral sugars were estimated by gas–liquid chromatography (GC-14A, Simadzu Corporation, Kyoto, Japan) of derived alditol acetates using inositol as internal standard . The column, SP-2330 fused silica (30 m × 0.32 mm × 0.25 mm), was maintained at 120°C for 2 min and then raised to 220°C at 25°C/min. N2 was used as the carrier gas (1 ml/min) with an injection volume of 1 ml. The concentrations of uronic acids in the hydrolysates were determined by the m-hydroxydiphenyl sulfuric acid method with a galacturonic acid standard .
Results and discussion
Preparation of the crude polysaccharides from skin juice, gel juice, and flower
Purification and composition of polysaccharides
Yield, molecular weight distribution, and sugar composition (mol%) of A. vera polysaccharides
Gel juice polysaccharides
Skin juice polysaccharides
Molecular weight distribution (kDa)
230 to 3,340
115 to 207
15 to 110
5 to 13
2 to 59
90 to 290
9 to 52
21 to 108
45 to 125
5 to 30
Molecular weight of each peak (kDa)
Using (50% N + 50% P + 50% K) fertilizer was the most effective in increasing the crude polysaccharide content of A. vera (75%). The effect of T150 N was not superior to the fertilizer in this experiment.
In the process of preparing A. vera, the leaf skin is usually disposed of as waste, and aloe flower is also underestimated due to the small amount of origin from A. vera. The results from this work indicate that a considerable amount of polysaccharides is present in the skin juice, which is 2.4 times the level in gel juice; thus, we suggest that A. vera skin should be used fully for the extraction of polysaccharides rather than discarded. A. vera flower also contains an abundant amount of polysaccharides. However, the concentration of carbohydrates detected in the first ethanol-precipitated solid from the skin juice was rather low. This could be owing to the presence of co-precipitated protein and possible oxalate materials. Also, the polysaccharide solution extracted from aloe flower was more contaminated with protein and colored materials or phenolic compounds; thus, additional purification steps were necessary to remove these materials. Neutral polysaccharides accounted for 59.1% and 79.8% of the total recovered polysaccharide preparations for the skin and gel juices, respectively, with small amounts of acidic polysaccharides obtained after DEAE-Sephadex A-25 anion-exchange chromatography. In contrast, the polysaccharides of A. vera flower were mainly composed of acidic polysaccharide (85.2%). After further purification by gel permeation chromatography, component sugar analysis by gas–liquid chromatography indicated that there were significant differences between the neutral polysaccharides and acidic polysaccharides from different tissue zones of A. vera. In the neutral polysaccharides from the gel juice and flower tissues, glucose was the largest component, which accounted for around 81% and 40%, respectively. Also, the neutral polysaccharide from the skin juice was composed mostly of galactose (62.8%). Additionally, in the acidic polysaccharides detected in the experiment from the gel juice and flower tissues, galactose and glucose were the major monosacccharides, while the acidic polysaccharide from the skin tissue was mainly consisted of glucose and mannose. These results were broadly similar to those obtained for the gel polysaccharides of A. vera by Hikino et al. ; on the contrary, Wozniewski et al.  found that mannose was the predominant sugar. Glucuronic acid was the major uronic acid in all acidic polysaccharides from different tissues.
This trend of increased polysaccharides due to increased application of fertilizer was also observed in the case of the total weight of leaves, aloe gel, and skin juice. The application of organic fertilizer increased the total weight of leaves and crude polysaccharides without hampering the nutrient uptake process, which provided better results due to better medicinal value. Further studies of the structure and biological role of these polysaccharides are necessary, and parts of them are in progress in our group.
The financial support of the National Institute of Genetic Engineering and Biotechnology (NIGEB), Iran, was greatly appreciated.
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