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Article

Valorization of Aloe vera Skin By-Products to Obtain Bioactive Compounds by Microwave-Assisted Extraction: Antioxidant Activity and Chemical Composition

by
Ignacio Solaberrieta
,
Alfonso Jiménez
and
María Carmen Garrigós
*
Department of Analytical Chemistry, Nutrition & Food Sciences, University of Alicante, San Vicente del Raspeig, ES-03690 Alicante, Spain
*
Author to whom correspondence should be addressed.
Antioxidants 2022, 11(6), 1058; https://doi.org/10.3390/antiox11061058
Submission received: 8 May 2022 / Revised: 24 May 2022 / Accepted: 25 May 2022 / Published: 26 May 2022
(This article belongs to the Special Issue Agri-Food Wastes as Natural Source of Bioactive Antioxidants)
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Versions Notes

Abstract

:
Aloe vera skin (AVS) is a major by-product of Aloe processing plants all over the world. In this study, response surface methodology was used to optimize microwave-assisted extraction (MAE) of bioactive compounds from AVS. The influence of extraction parameters, such as ethanol concentration (%Et), extraction temperature (T), time (t) and solvent volume (V), on extraction yield (Y), total phenolic content (TPC), antioxidant activity (DPPH and FRAP methods) and aloin content, was studied. Optimum extraction conditions were determined as 80% ethanol, 80 °C, 36.6 min and 50 mL and optimized extracts showed interesting contents of polyphenols and antioxidant performance. The phenolic profile was determined by HPLC-DAD/MS and some major phenolic compounds, such as aloin A, aloin B, aloesin, aloe-emodin, aloeresin D, orientin, cinnamic acid and chlorogenic acid, were quantified while eight other compounds were tentatively identified. Moreover, structural and thermal properties were studied by FTIR and TGA analyses, respectively. The obtained results suggested the potential of AVS as a promising source of bioactive compounds, thus increasing the added value of this agricultural waste.

Graphical Abstract

1. Introduction

In recent decades, growing environmental concerns combined with the imminent depletion of fossil fuels have encouraged the concept of the circular economy as an environmentally friendly approach to prevent waste generation in productive processes, as well as to develop natural-based products in order to reduce dependence on fuel-based materials [1]. The use of biopolymers or active biomolecules obtained from agricultural by-products or wastes has gained major importance in many countries around the world due to its environmental and economic advantages [2]. Recent studies have reported a wide variety of agrowastes as renewable sources of bioactive compounds or biopolymers that are currently underexploited, such as Aloe vera skin [3,4], cocoa bean shells [5], tomato seeds [6] and carob pod bark [7], among many others.
Aloe vera has been associated with curative or healing-promoting properties since ancient times. Several studies have demonstrated its anticancer, antiviral, anti-inflammatory, antimicrobial and antioxidant activities [8,9]. Pharmaceutical, food and cosmetic industries have used Aloe vera in innumerable product formulations which have been continuously growing in recent years [10,11]. The most valuable part of the plant is the inner leaf gel, which is used for product manufacturing. In Aloe vera processing plants, the inner gel is generally separated from the external skin, which accounts for over 30% of the total leaf weight, generating large amounts of waste. In most cases, this agrowaste lacks commercial use and is usually discarded, used as compost or directly incinerated [12]. Even though there is little information about Aloe vera skin compared to the inner gel, which has been extensively studied, it has been reported that Aloe vera skin could be a promising source of bioactive compounds which might be used in food, food packaging or biomedical applications [4,13,14].
There is a general consensus that biological activities of medicinal plants, including Aloe vera, which present very complex phytochemical profiles and many constituents, should be ascribed to the synergistic action of several compounds rather than to a single molecule. More than 75 active compounds have been identified in Aloe vera, with some of them, such as polysaccharides, related to wound healing, anti-inflammatory and antidiabetic activities [8,15]. However, the specific roles of other components have not been completely elucidated yet and some of them are suspected to be responsible for undesirable effects when consumed. This is the case with aloin, an anthraquinone-C-glycoside which is present, especially, in the latex of Aloe vera leaves and naturally occurs as a mixture of diastereoisomers, aloin A and aloin B [16]. Even though some studies have highlighted some protective benefits of anthraquinones, such as hepatoprotective, anticancer, antimicrobial and antioxidant activities [17,18,19], it has been reported to have a strong laxative effect, and it might cause other undesirable effects [20,21]. The maximum content of aloin in products intended for oral consumption is limited by specific regulations such as in North America, where the International Science Aloe Council has set a limit of 10 ppm of aloin A and B [20]. On the other hand, the European Council Directive 88/388/EEC established an aloin limit of 0.1 ppm in flavorings for beverages [22].
The extraction of bioactive molecules from plants could be carried out by using a variety of methods [23]. In recent years, several non-conventional and more environmentally friendly extraction techniques, which usually lead to higher overall extraction yields with less time and solvent consumption, have been developed [24,25]. Among them, microwave-assisted extraction (MAE) has gained importance due to its multiple advantages compared to conventional extraction techniques [26,27]. The synergistic combination of heat and mass transfer phenomena, in which both gradients work in the same direction, combined with volumetric heat dissipation inside the irradiated medium, are the most distinctive characteristics of MAE [28]. Moreover, it has been reported that this heating mechanism generates internal pressure into the plant materials, contributing to the rupture of cell walls and promoting solvent penetration into the vegetal matrix. Therefore, active compounds could be easily solubilized and extracted [28].
Most plant extracts comprise complex mixtures of different phytochemical constituents with diverse chemical structures, and their analysis remains challenging. Currently, several literature reviews on the identification and quantification of active compounds extracted from plants are available [29,30,31]. Even though some analytical techniques, such as gas chromatography and capillary electrophoresis, have been employed, high performance liquid chromatography (HPLC) combined with mass spectrometry (MS) has been by far the most frequently used technique for the identification and quantification of secondary metabolites extracted from plants [32,33,34,35]. Successful phenolic profiling strongly relies on proper optimization of chromatographic conditions, which are crucial for the selection of adequate mobile phases and gradient elution programs.
MAE has been used to extract bioactive compounds from several agrowastes [36]. However, to the best of our knowledge, no studies have been carried out for the MAE optimization of bioactive compounds with antioxidant activity from Aloe vera skin, adding value to this underexploited renewable resource. In this context, this work aimed at optimizing a new extraction procedure for bioactive compounds from Aloe vera skin in order to increase the added value of this agricultural waste. The optimal MAE conditions for maximizing the recovery of active phenolic compounds and the antioxidant activity of the extracts were determined. The influence of four extraction variables (irradiation time, extraction temperature, ethanol concentration in the extraction solvent and volume) was studied and the MAE process was optimized using a Box-Benhken design (BBD). Total phenolic content (TPC), antioxidant activity by DPPH and FRAP methods and aloin content in Aloe vera skin extracts were evaluated as the response variables. Moreover, phenolic profile, thermal and structural properties of the optimized Aloe vera skin extract were also determined by HPLC-DAD/MS, thermogravimetric analysis (TGA) and Fourier transform infrared spectroscopy (FTIR), respectively. Finally, morphological changes on the AVS structure due to the MAE process were studied by scanning electron microscopy (SEM).

2. Materials and Methods

2.1. Reagents and Raw Materials

Sodium carbonate, Folin-Ciocalteu reagent (2 N), 2,2-diphenyl-1-picrylhydrazyl (DPPH), sodium acetate, glacial acetic acid, hydrochloric acid, 2,4,6-tripyridyl-s-triazine (TPTZ), ferric chloride hexahydrate, gallic acid, 6-hydroxy-2,5,7,8-tetramethylchroman-2-carboxylic acid (Trolox), ethanol (absolute grade), methanol, acetonitrile (HPLC grade), formic acid and cinnamic acid were purchased from Sigma Aldrich (Madrid, Spain). Aloin A, aloin B, orientin, aloeresin D, aloesin and aloe-emodin were acquired from Cymit Química (Barcelona, Spain). Chlorogenic acid and all other phenolic standards used in this study were purchased from Extrasynthese (Genay, France). Ultrapure water from a Millipore Milli-Q system was used (18.2 MΩ·cm at 25 °C).
Fresh Aloe vera leaves, from three-year old plants, were kindly supplied by Las Coronas (Carnota, Seville, Spain), and they were thoroughly washed with distilled water to remove the adhering soil particles and other contaminants. Then, leaves were weighted and measured for their length, thickness and width (Table 1). Subsequently, the base, tip and spikes were removed, and the epidermis was carefully separated from the inner gel using a sharp knife. The yield of Aloe vera waste was determined and expressed as a fraction of the total leaf weight. The resulting Aloe vera skin was intensively washed with distilled water and the residual gel was removed. Then, it was cut into small pieces and frozen at −80 °C. Afterwards, the skin was freeze-dried with a Telstar Lyoquest—55 PLUS (Terrassa, Barcelona, Spain) and ground using a ZM 200 high-speed rotatory mill (Restch, Hann, Germany). Particles passing through a 1.0 mm sieve were used to ensure the homogeneity of the sample. Finally, the freeze-dried Aloe vera skin powder (AVS) was vacuum packed and stored in the darkness until further analysis.

2.2. AVS Characterization

AVS characterization was carried out by following AOAC official methods [37] and reported works for the analysis of similar plant materials [3,38]. Total content of lipids was gravimetrically determined after 8 h of Soxhlet extraction using petroleum ether. The crude protein content was calculated using the Kjeldahl method by multiplying the nitrogen value by 6.25. Total ash was determined by incineration in a muffle at 550 °C for 4 h. The moisture content was determined after skin separation by freeze-drying. All analyses were carried out in triplicate.

2.3. Microwave-Assisted Extraction (MAE)

MAE was performed using a Milestone flexiWAVETM microwave oven (Milestone srl, Bergamo, Italy) in the open vessel configuration, and the solvent was heated and refluxed through the sample. Ethanol:water mixtures were used as reported efficient solvents for the extraction of phenolic compounds from plant materials [7,39,40], with ethanol showing low toxicity [41]. According to preliminary tests, the AVS amount was fixed at 1.5 g. The initial heating rate was optimized and held constant among the different extraction experiments. During the extraction process, samples were stirred at 400 rpm and different combinations of solvent composition (%Et), extraction temperature (T), extraction time (t) and volume (V) were used according to Table 2. After extraction, the obtained Aloe vera skin extracts (AVE) were cooled to room temperature and centrifuged at 5300 rpm for 10 min. The solid residue was washed twice with the extraction solvent and then discarded. Then, the supernatant was pooled with the washing solvent and stored overnight at −20 °C in order to remove possible interferences by precipitation. After that, the precipitates were removed by centrifugation at 5300 rpm and 4 °C for 10 min. The supernatant was collected, and the ethanol was subsequently evaporated under reduced pressure. Afterwards, the extract was frozen at −80 °C, freeze-dried until completely dry and finally stored in vacuum-sealed packs at −20 °C in darkness until further analysis. AVE solutions were freshly prepared, before analysis, at 500 mg kg−1 in ethanol:water (40%, v/v).

Box-Behnken Experimental Design (BBD)

MAE optimization of bioactive compounds from AVS was performed by using a BBD with 29 runs and 5 central points in order to maximize extraction yield, total phenolic content (TPC) and antioxidant activity (DPPH and FRAP), as well as to minimize aloin content. The effect of four independent variables (ethanol concentration (%Et: 40–80%, v/v), temperature (T: 40–80 °C), time (t: 5–40 min) and solvent volume (V: 50–80 mL)) were investigated at three levels. All experimental runs were performed randomly to minimize the effect of unexpected variability in the response variables. The range of the studied independent variables was selected on the basis of preliminary experiments (data not shown), experimental limitations, constructive characteristics of the used equipment and previously reported information in the literature.
Response surface methodology (RSM) was used, and the following second-order polynomial model was applied for regression analysis of the experimental data:
Y =   β 0 + ∑   β i X i + ∑   β i X i 2 + ∑   ∑   β ij X i X j
where Y represents the predicted response variable; Xi and Xj represent the independent variables; β0 is a constant coefficient and βi, βii, βij are the regression coefficients of the linear, quadratic and interaction effect terms, respectively. The lack of fit test and coefficient of determination (R2) were used to determine the adequacy of the model to predict experimental data. Statistical significance of the model parameters was determined at 5% probability level (α = 0.05), and graphic analysis of the principal effects and interactions of independent variables on the studied responses was used.

2.4. AVE Characterization

2.4.1. Extraction Yield

The extraction yield was gravimetrically determined by using the following equation:
Yield   ( % ) = 100   m AVE m AVS
where mAVE is the weight of the extract obtained after freeze-drying and mAVS is the weight of the dried starting material.

2.4.2. Total Phenolic Content (TPC)

The total phenolic content of AVE was determined using the Folin-Ciocalteu assay according to Lucini et al. [4] with slight modifications. Aliquots (0.5 mL) of each extract were mixed with 2.5 mL of the Folin-Ciocalteu reagent, previously diluted in distilled water (1:10, v/v), and added with 2.0 mL of 7.5 wt% aqueous sodium carbonate. Then, the mixture was vortexed, and the absorbance was recorded at 765 nm after 30 min of incubation at 45 °C in the dark using a Biomate 3 UV-vis spectrophotometer (Thermospectronic, Mobile, AL, USA). Gallic acid in EtOH:H2O (40%, v/v) was used as a reference standard for quantification (5–80 mg kg−1, R2 = 0.9995). The results were expressed as milligrams of gallic acid equivalents (GAE) per gram of AVE. Each extract was analyzed in triplicate.

2.4.3. Antioxidant Activity

2.4.3.1. DPPH Radical Scavenging Assay

The DPPH scavenging activity of AVE was determined, in triplicate, as described in previous studies [42,43,44] with some modifications. Briefly, 0.3 mL of AVE were mixed with 2.2 mL of a freshly prepared DPPH solution (10−4 mol L−1 in ethanol). The mixture was vortexed and incubated at room temperature in the dark for 90 min. Preliminary studies demonstrated that this amount of time was required to accomplish the reaction and reach the steady state. Then, absorbance was measured at 517 nm against a pure ethanol blank. Trolox in EtOH:H2O (40%, v/v) was used as the reference standard for quantification (5–70 mg kg−1, R2 = 0.9994). Results were expressed as milligrams of trolox equivalents (TE) per gram of AVE.

2.4.3.2. FRAP Assay

The ability of AVE to reduce a ferric-tripyridyltriazine complex to its ferrous form was assessed according to Benzie and Strain [45]. FRAP reagent was prepared by mixing 0.3 mol L−1 acetate buffer (pH = 3.6), 10 mmol L−1 TPTZ made up in 40 mmol L−1 HCl and 20 mmol L−1 FeCl3 at a 10:1:1 ratio. Then, 0.1 mL of AVE were mixed with 3 mL of the freshly prepared FRAP reagent pre-warmed at 37 °C. The mixture was vortexed, and the absorbance was measured at 593 nm after 30 min of incubation at 37 °C in the darkness. Trolox in EtOH:H2O (40%, v/v) was used as the reference standard (5–100 mg kg−1) (R2 = 0.9996). The results were expressed as milligrams of trolox equivalents (TE) per gram of AVE. Each extract was analyzed in triplicate.

2.4.4. Aloin Content Determination

The total aloin content (A and B stereoisomers) in AVE was determined as described by Brown et al. [46] with slight modifications. An Agilent series 1260 Infinity Quaternary HPLC system (Agilent Technologies, Palo Alto, CA, USA) equipped with a diode array detector was used. Chromatographic separation was achieved with a Teknokroma Brisa LC2 C18 column (150 × 4.6 mm I.D. × 5 µm film thickness). Then, 15 µL of samples were injected, and a gradient of eluent A (water) and eluent B (acetonitrile) was used. The flow rate was 1.0 mL min−1 and gradient elution conditions applied were: 17% B for 8 min followed by a linear gradient to 100% B in 20 min (held 1 min), followed by a linear gradient to 17% B in 5 min. Standard solutions were freshly prepared for quantification of aloin A and B (0.005–100 mg kg−1, R2 = 0.9998). All samples were filtered through 0.45 µm pore size nylon membrane filters prior to HPLC analysis at 357 nm. Triplicate runs were carried out for each sample. Linearity, limit of detection (LOD), limit of quantification (LOQ) and precision were determined to validate the analytical method.

2.5. Characterization of AVE Obtained under Optimum Conditions

2.5.1. Attenuated Total Reflectance-Fourier Transform Infrared Spectroscopy (ATR-FTIR)

The FTIR spectrum of AVE was recorded by using an infrared spectrophotometer JASCO FTIR 4700 IRT-5200 (Easton, MD, USA) in the 4000–500 cm−1 range with a spectral resolution of 4 cm−1 and 32 scans. The attenuated total reflectance (ATR) mode was used with a Golden Gate accessory equipped with diamond crystal, and tests were performed in triplicate.

2.5.2. Thermogravimetric Analysis (TGA)

The TGA of AVE was carried out using Mettler Toledo TGA/SDTA 851e equipment (Schwarzenbach, Switzerland). Approximately 5 mg of the sample were heated from room temperature to 700 °C at 10 °C min−1 under nitrogen atmosphere (50 mL min−1) using alumina pans. The analysis was performed in triplicate.

2.5.3. AVE Phenolic Profile

2.5.3.1. HPLC-MS Qualitative Analysis

The identification of phenolic compounds present in AVE was performed by high-performance liquid chromatography coupled to mass spectrometry (HPLC-MS) according to Lee et al. [47] and Quispe et al. [48], with some modifications. An Agilent 1100 HPLC system equipped with a quaternary solvent delivery system coupled to an LC/MSD ion trap mass spectrometer with electrospray ionization (ESI) source (Agilent Technologies, Palo Alto, CA, USA) was used. Chromatographic separation was performed on a HALO C18 column (100 mm × 4.6 mm I.D. × 2.7 µm) coupled to a HALO C18 guard column 90 Å (4.6 × 5 mm I.D. × 2.7 µm) operating at 25 °C. The mobile phase was composed of two solvents added with 0.1% formic acid (A: water, B: acetonitrile). The gradient elution program was as follows: linear gradient from 10% B to 40% B in 20 min followed by a linear gradient to 98% B in 5 min (held 5 min). The flow rate was 0.3 mL min−1 and the injection volume 6 µL. MS spectra were recorded in the range 50–900 m/z in negative ionization mode. The electrospray chamber was set at 3.5 kV with a drying gas temperature of 350 °C. The N2 pressure and flow rate of the nebulizer were 50 psi and 10 L min−1, respectively.
AVE and standard solutions of phenolic compounds were freshly prepared in methanol and filtered through a 0.22 µm nylon membrane prior to injection. Extracted ion chromatograms and mass spectra experimental data were used for identification of polyphenols in AVE through comparison with the standards. Other phenolic compounds also present in AVE were tentatively identified based on the information of ion fragments and reported literature.

2.5.3.2. HPLC-DAD Quantitative Analysis

Quantitative analysis of previously identified compounds by HPLC-MS was carried out by HPLC-DAD. An Agilent series 1260 Infinity Quaternary LC HPLC system (Agilent Technologies, Palo Alto, CA, USA) equipped with a diode array detector was used. Operating conditions detailed in Section 2.5.3.1 were applied, and simultaneous monitoring was set at 254 nm (aloesin and aloe-emodin), 270 nm (cinnamic acid), 324 nm (chlorogenic acid) and 357 nm (orientin, aloin B and aloin A) for quantification. The optimal detection wavelength of each compound was set by previously verifying the obtained UV spectra. Quantitative analysis was performed using the external calibration method based on the preparation of calibration curves at ten concentration levels for the aforementioned standard compounds in methanol. All analyses were carried out in triplicate. Linearity, limit of detection (LOD), limit of quantification (LOQ) and precision (RSD) were determined to validate the analytical method.

2.6. Scanning Electron Microscopy (SEM)

SEM was employed to evaluate the damage in the vegetal material produced by the MAE process. Raw and extracted AVS freeze-dried samples were mounted on aluminum stubs and then coated with a gold layer under vacuum using an SCD 004 Balzers sputter coater (Bal Tec., AG, Furstentum, Liechtenstein). SEM analysis was carried out using a JEOL JSM 840 scanning electron microscope (Peabody, MA, USA) at an accelerating voltage of 15 kV and 2500× magnification level.

2.7. Statistical Analysis

Statgraphics Centurion XVI (Statistical Graphics, Rockville, MD, USA) was used to generate and analyze the BBD results. Graphic analysis of the principal effects and interactions between variables was used to interpret the results. The coefficients of quadratic polynomial models were determined by data regression analysis and the adequacy of the fitted models was determined by evaluating the lack of fit, coefficient of determination (R2), and F test obtained from the analysis of variance (ANOVA). The statistical significance of the model parameters was determined at a 95% probability level (α = 0.05).

3. Results and Discussion

3.1. AVS Characterization

The dimensions of Aloe vera leaves used in this work (Table 1) were very similar to the morphological characteristics of plants studied by Zapata et al. [49]. Even though other authors reported different dimensions for three- or four-year old Aloe vera plants [3,38,50], it is well known that many factors, such as environmental and soil conditions, water availability and plant variety, could significantly influence plant growth, thereby leading to different leaves in terms of size and phytochemical constituents [51]. In this case, after tissue separation of Aloe vera leaves, the yields of skin and other components of the residue, such as the tip, base and spikes, accounted for up to 15.1 ± 2.1% and 17.5 ± 4.1%, respectively. These results are in close agreement with those found by Femenia et al. [38] and Flores-López et al. [3], who reported very similar yields for the epidermis fraction in Aloe vera plants. Several drying techniques, including freeze drying, air drying and oven drying at different temperature and time programs, were tested in order to find the most suitable drying process to avoid leaf browning, which might be directly related to oxidative processes and detrimental effects on bioactive substance content in plants. Similar to Ng et al. [52], freeze drying was selected as the most adequate drying process and no apparent oxidation of AVS was observed. On the other hand, it is well known that a smaller particle size will enhance solute–solvent interaction during the extraction process; but too many fine particles might make subsequent separation steps difficult. In this work, particles passing through a 1.0 mm sieve were used.
The physicochemical characterization results of AVS are shown in Table 1. Moisture, ash, protein and fat contents of AVS resulted in close agreement with experimental data reported in other studies [3,12,38]. Proteins and lipids represented a minor fraction of AVS, accounting for 6.5 ± 0.2 wt% and 2.4 ± 0.1 wt%, expressed on a dry matter basis, respectively. On the other hand, the ash content was relatively high, and it accounted for 15.5 ± 0.1%. It has been reported that calcium, potassium, sodium and magnesium are the main mineral components present in AVS ash. It has also been suggested that the presence of minerals in Aloe vera is essential for the proper functioning of enzymatic systems and for improving resistance against microorganisms and water stresses. The mineral content found in AVS was much more concentrated compared to other plant tissues, such as gel or flowers [3]. Apart from these components, it has also been reported that AVS is an interesting source of polysaccharides [53] and lignocellulosic matter [12]. Moreover, Lucini et al. [4] and Quispe et al. [48] reported that AVS is rich in phenolic compounds and its extracts exhibit antioxidant activity to a higher degree than other parts of the plant. In this sense, AVS represents a low-cost, underused biomass resource with high potential to be valorized, finding a wide range of applications in cosmetic, food or medicinal products.

3.2. MAE Optimization

3.2.1. Model Fitting and Analysis

The optimization of MAE conditions for the extraction of polyphenols from a wide variety of plant leaves, such as Myrtus communis L. [54], Achillea millefolium [55], strawberry [56], Vitis vinifera L. [57] and artichoke [58], has been reported in recent years by using response surface methodology (RSM). Even though these vegetal matrices might have results similar to Aloe vera leaf skin, optimized MAE conditions could not be generalized to all plant materials due to the diverse nature of the existing bioactive phytochemicals and the different levels of interaction between microwave irradiation and different plants and vegetable parts. Moreover, it is well known that the MAE of bioactive compounds from plant materials could be affected by a wide number of experimental factors; in consequence, MAE optimization should be performed in each study. In this work, the influence of ethanol concentration (%Et), extraction temperature (T), extraction time (t) and solvent volume (V) on the MAE of bioactive compounds from AVS was studied by using a Box-Behnken experimental design with 29 independent runs, including 5 central points, which were performed randomly. The experimental conditions and data obtained in terms of extraction yield, TPC, antioxidant activity (DPPH and FRAP assays) and total aloin content are shown in Table 2.
Multiple regression analysis was applied to the experimental data, and all the studied responses were fitted to second-order mathematical models as a function of the independent factors. The resulting models are presented in Equations (3)–(7).
Extraction   yield = − 23.762 + 0.512   A   + 0.122   B   + 0.326   C   + 0.824   D   − 0.004   A 2 + 0.000   AB   − 0.002   AC     − 0.003   A   D   − 0.002   B 2 − 0.001   BC   + 0.002   BD   − 0.001   C 2 − 0.001   CD   − 0.005
TPC = 98.296 + 0.533   A   − 0.245   B   − 0.952   C   − 0.295   D   + 0.001   A 2 + 0.001   AB   − 0.004   AC     + 0.002   AD   − 0.001   B 2 + 0.009   BC   + 0.001   BD   − 0.006   C 2 + 0.014   CD   − 0.002   D 2
DPPH = 52.525 + 0.123   A   − 0.575   B   − 0.439   C   + 0.504   D   + 0.004   A 2 − 0.002   AB   − 0.0025   AC     − 0.003   AD   + 0.006   B 2 + 0.011   BC   − 0.003   BD   − 0.006   C 2 + 0.002   CD   − 0.002   D 2
FRAP = 193.053 − 0.317   A   − 0.490   B   − 1.384   C   − 2.129   D   − 0.001   A 2 + 0.001   AB   + 0.014   AC     + 0.012   AD   + 0.005   B 2 + 0.009   BC   − 0.007   BD   − 0.006   C 2 + 0.006   CD   + 0.013   D 2
aloin = 56.258 − 0.066   A   − 0.037   B   − 0.340   C   − 0.455   D   + 0.003   A 2 − 0.003   AB   + 0.005   AC     + 0.002   AD   + 0.003   B 2 + 0.003   BC   − 0.003   BD   − 0.004   C 2 + 0.001   CD   + 0.004   D 2
where A, B, C and D represent ethanol concentration, extraction temperature, extraction time and solvent volume, respectively.
In order to study the effect of the experimental factors in the response variables as well as to evaluate the adequacy of the fitted models, analysis of variance (ANOVA) was carried out and results are summarized in Table 3. The coefficient of determination (R2) values and the p-values obtained for lack of fit test were used as a measurement of the degree of fitness of the proposed models to the experimental data. As shown in Table 3, non-significance of the lack of fit test (p > 0.05) and acceptable R2 values were obtained in all cases, accounting for 0.9498, 0.9308, 0.8691, 0.9329 and 0.9354 for yield, TPC, DPPH, FRAP and aloin content, respectively. These values indicate the percentage of variability being explained by the models for each response (87 to 95%), highlighting a high level of correlation between the experimental data and predicted values. Moreover, adjusted R2 values did not differ greatly from R2 ones, and in all cases, the distribution of residuals was randomly scattered around zero. These results confirmed the reliability of the models to be used in subsequent optimization stages.

3.2.2. Effect of Extraction Variables on the Extraction Yield

The extraction yield ranged from 18.2 to 26.3 g AVE 100 g AVS−1 under the 29 experiments performed (Table 2). According to Table 3, ethanol concentration and solvent volume had significant effects (p < 0.05) on extraction yield, with the former being the most significant factor by far. Moreover, three quadratic effects (A2, B2 and D2) also showed significant effects (p < 0.05). Particularly, ethanol concentration and all mentioned quadratic effects had negative effects, while solvent volume showed a positive effect. Consequently, significantly higher extraction yields were obtained at a low ethanol concentration level. Solvent constitution is directly related to the type and quantity of compounds extracted from plant materials. In this case, a low ethanol concentration might favor the co-extraction of other untargeted plant components apart from polyphenols. It has been reported that increasing water content in the extraction solvent resulted in higher polarity, which might enhance the extraction of other polar compounds from AVS such as polysaccharides [59]. Furthermore, water addition can be used to improve solvent penetration into vegetal sample matrices as well as to enhance heating efficiency, usually leading to higher extraction yields [26]. On the other hand, extraction yield was significantly affected (p < 0.05) by the solvent volume. A positive effect was observed, so the higher the solvent volume, the higher the obtained extraction yield. A low amount of solvent usually promotes mass transfer barriers, which limit the movement of compounds out of the vegetal matrix since active compounds are concentrated in certain regions near the vegetal surface [26]. On the contrary, larger extraction volumes can cause more efficient swelling of plant materials, enhancing the extraction procedure due to an easier rupture of the cell walls. However, in the case of MAE, an excessive amount of solvent may cause poor microwave heating efficiency as the majority of the irradiation would be absorbed by the solvent instead of the plant material and additional power might be needed to obtain higher yields.

3.2.3. Effect of Extraction Variables on Total Phenolic and Aloin Contents

TPC and aloin content obtained under the 29 experiments carried out in the BBD varied from 86.5 to 125.8 mg GAE g AVE−1 and from 36.5 to 57.5 mg g AVE−1, respectively (Table 2). ANOVA analysis (Table 3) showed that total phenolic content was significantly (p < 0.05) influenced by the ethanol concentration and the interaction between extraction time and solvent volume, both with positive effects, while the aloin content was only significantly affected (p < 0.05) by the ethanol concentration, also with a positive effect. Several authors reported that high ethanol concentrations in the extraction solvent were adequate for obtaining extracts with high TPC or antioxidant activities from aloe [4,13,43,44,60] and other plant materials [40,55,61]. The solubility of phenolic compounds is strongly related to their chemical nature and polarity. By increasing ethanol content in the extraction solvent, the solubility of certain polyphenols resulted in enhanced and, consequently, higher TPC and antioxidant activities, as expected. The significant interaction effect (p < 0.05) between extraction time and solvent volume on the TPC response is shown in Figure 1a. It was observed that the combination of short extraction times and low solvent volumes resulted in higher TPC values. Similar results were found by other authors who reported that the increase in the exposure time of the sample to microwave irradiation might promote the extraction of other components, apart from polyphenols, from plant materials, causing a relative decrease in TPC values on extracts [55,62]. Furthermore, microwave irradiation time may lead to thermal degradation and oxidation of sensitive compounds such as some polyphenols.

3.2.4. Effect of Extraction Variables on Antioxidant Activity

The antioxidant activity, expressed as DPPH radical scavenging activity, varied from 49.9 to 73.4 mg TE g AVE−1 in the 29 MAE experiments carried out in this study (Table 2). DPPH radical scavenging activity was significantly affected (p < 0.05) by three linear effects (ethanol concentration, extraction temperature and solvent volume), three quadratic effects (B2, C2 and A2) and one interaction effect (BC). The linear effects of the ethanol concentration and extraction temperature were positive, while the solvent volume showed a negative effect. Furthermore, all quadratic effects were positive except for extraction time. Overall, the DPPH radical scavenging activity increased with increasing ethanol concentration and extraction temperature, while decreasing solvent volume. Moreover, the interaction effect between the extraction temperature and time showed a significant (p < 0.05) positive effect on DPPH antioxidant activity. As shown in Figure 1b, an increase in extraction time at low extraction temperature values led to a decrease in DPPH antioxidant activity of the extract, whereas increasing extraction time at high extraction temperatures led to enhanced DPPH values. Overall, higher antioxidant activity was obtained at 80 °C and 40 min. It is well known that polyphenols could exert antioxidant activity and many other interesting properties [63]. In this case, similarly to TPC, a high ethanol concentration favored the extraction of certain components which might act as proton-donor substrates, scavenging the radicals which are involved in DPPH reactions and contributing to the antioxidant activity of AVE. On the other hand, high extraction temperatures caused a drop in viscosity and surface tension, enhancing the capacity of the extraction solvent to penetrate the vegetal matrix, resulting in an increase in the solubility of the target compounds [26]. In addition, cell walls might be damaged by the action of high temperatures during the extraction process, which could favor the release of active compounds in the extraction solvent [26,28]. However, it has been reported that some phenolic compounds might suffer thermal degradation when exposed to high temperatures [64], and optimal temperatures for MAE usually do not exceed 100 °C.
Concerning the antioxidant activity estimated by the FRAP method, the obtained values ranged from 90.5 to 134.1 mg TE g AVE−1 under the 29 experiments performed in the BBD (Table 2). FRAP values were significantly influenced (p < 0.05) by the linear effect of the solvent concentration and extraction time, quadratic effect of solvent volume and interaction effects of AC and AD. Overall, the significant effects (p < 0.05) were positive, resulting in enhanced FRAP antioxidant activity values by increasing ethanol concentration in the extraction solvent, extraction time and solvent volume. Moreover, the response surface plots of the interaction effects between the ethanol concentration and extraction time and solvent volume are shown in Figure 1c,d, respectively. A slight decrease in FRAP values was observed with increasing extraction time at low ethanol concentrations in the extraction solvent. However, FRAP antioxidant activity was enhanced with increasing extraction time at high ethanol concentrations. Similar behavior was observed for the interaction effect between the ethanol concentration and solvent volume. Altogether, higher FRAP values were obtained at high ethanol concentration levels and long extraction times as well as high solvent volumes.
As already detailed for TPC and DPPH values, a high ethanol concentration also favors the extraction of some components, which contributes to enhancing FRAP antioxidant activity. Similar to the extraction temperature, higher extraction times contribute to cell wall degradation and liberation of active compounds into the extraction solvent, increasing the antioxidant activity of the extracts. On this point, it is worth mentioning that different methods used to determine the antioxidant activity of AVE might evaluate different fractions of antioxidant compounds, which might be partially overlapped. On the one hand, the FRAP method evaluates the content of electron-donating species with a certain redox potential, whereas the DPPH method assesses the free radical scavenging capacity of a sample [43]. Moreover, the steric accessibility of DPPH radicals is a major aspect of the reaction, as this method is much more sensitive to small molecules, and many large antioxidant compounds might hardly participate in this reaction [65]. This effect was already highlighted by Kim et al. [43], who extracted polyphenols and antioxidant compounds from Aloe vera gel, and they observed that the antioxidant activity of aloe extracts evaluated by the DPPH method may be underestimated to a certain degree.

3.2.5. Optimal Extraction Conditions

Table 4 shows the experimental conditions which optimized each response variable individually and the optimum predicted values by the studied models. Great variability was found among the different sets of experimental factors which maximized each response variable, as expected from the analysis of linear, quadratic and interaction effects of the extraction variables. Consequently, it was not possible to clearly determine the best extraction conditions for AVS only considering these results. For this reason, a simultaneous optimization procedure using the desirability function was carried out to find the experimental conditions which simultaneously satisfy all the requirements for each response. First, the optimization was performed in order to simultaneously maximize extraction yield, TPC, DPPH and FRAP and minimize aloin content. However, due to the dissimilar extraction conditions summarized in Table 4, a quite low desirability value was obtained (0.5802) and further approaches were considered. According to ANOVA analysis (Table 3), the ethanol concentration was by far the most significant (p < 0.05) factor affecting all responses. Moreover, it exhibited a strong negative effect on the extraction yield with the optimum at 40%, whereas its effect was positive in all the other responses with an optimum at 80%. These results indicated an inverse correlation between extraction yield and the rest of the responses, suggesting that MAE conditions leading to high extraction yields could not be selective for polyphenol extraction. A similar scenario was described by Kim et al. [43] and Milutinovic et al. [66], who optimized the MAE of antioxidants from Aloe vera gel and Equisetum arvense waste, respectively. In this sense, considering that extraction yield could be interfered with by the co-extraction of other untargeted compounds and that TPC and antioxidant activity responses are usually directly correlated with phenolic compound concentrations, the extraction yield from the multi-response optimization was excluded.
In addition, it has been reported that aloin contributes to some extent to the antioxidant capacity exhibited by extracts from different aloe species [4,47,67]. Consequently, maximization of antioxidant activity and total phenolic content while simultaneously minimizing aloin content might lead to unavoidably low desirability values (0.5951). Therefore, multiresponse optimization was finally performed, maximizing TPC, DPPH, FRAP and aloin content and obtaining a desirability value of 0.8777, with optimal extraction conditions of 80% ethanol, 80 °C, 36.6 min and 50.0 mL. Subsequent purification or selective extraction steps could be implemented in the case of limitations regarding aloin content.

3.2.6. Verification Test under Optimum Extraction Conditions

The predicted values determined at a 95% level of probability for response variables obtained after multiresponse optimization in terms of extraction yield, TPC, DPPH, FRAP and aloin content were 16.0 ± 2.2 g AVE 100 g AVS−1, 118.4 ± 11.9 mg GAE g AVE−1, 74.2 ± 8.4 mg TE g AVE−1, 134.8 ± 12.0 mg TE g AVE−1 and 56.6 ± 5.6 mg aloin g AVE−1, respectively. Verification experiments under the obtained optimal conditions were carried out, in triplicate, and the obtained experimental responses regarding extraction yield, TPC, DPPH, FRAP and aloin were 17.3 ± 0.1 g AVE 100 g AVS−1, 116.4 ± 4.5 mg GAE g AVE−1, 69.0 ± 1.9 mg TE g AVE−1, 131.9 ± 6.5 mg TE g AVE−1 and 55.6 ± 0.2 mg aloin g AVE−1, respectively. Experimental results not significantly differing (p > 0.05) from predicted values were obtained in all cases. Moreover, reproducibility of the whole AVE extraction and characterization process was demonstrated, obtaining relative standard deviations ranging from 0.36 to 4.92% for all analyzed response variables. Additionally, it was observed that TPC, FRAP and aloin content in optimized AVE were almost higher than every individual run of the design, while DPPH was surpassed by only one experiment (Table 2). Regarding extraction yield, a value near 17% was obtained, as expected, due to the high ethanol concentration used in the extraction solvent. In conclusion, the obtained quadratic models were reliable for optimizing the extraction of bioactive compounds from Aloe vera skin in the studied experimental domain, resulting in a high degree of correlation between the experimental data and predicted values, indicating that the developed models could be used to predict the studied responses.
Compared to conventional extraction techniques, MAE’s major advantages are its high reproducibility and the noticeable reduction in extraction time and solvent consumption [26]. For instance, Sultana et al. [60] studied the effect of the extraction solvent on the yield of antioxidant compounds from different plant materials using conventional extraction techniques. They found that reflux extraction of Aloe barbadensis leaves with 200 mL of 80% ethanol accounted for 18.1 ± 0.7 g 100 g DW. However, a much longer extraction time of 6 h was required. In another work, Quispe et al. [48] reported an extraction yield of 16.2 g 100 g of AVS for a phenolic-enriched extract obtained after maceration with methanol for 48 h.

3.3. Characterization of AVE Obtained at Optimal Extraction Conditions

3.3.1. FTIR Analysis

It has been reported that Aloe vera plants contain a wide variety of bioactive compounds, including phenolic acids and derivatives, flavonoids, chromones, anthraquinones, polysaccharides and fatty acids. The FTIR–ATR spectrum of AVE obtained under optimal extraction conditions is shown in Figure 2a. The broad peak observed around 3275 cm−1 was attributed to the stretching vibration of different –OH groups of phenolic compounds such as flavonoids, anthraquinones and chromones [68,69]. The bands at 2925 and 1379 cm−1 might be assigned to C-H stretching and bending vibration of aliphatic hydrocarbons, respectively [68,70,71]. The absorption band at 1714 cm−1 was associated with C=O stretching, indicating the presence of carbonyl functional groups [70,72]. Peaks observed at 1222 and 877 cm−1 might be related to the stretching of C-O-C bonds of acetyl groups of esters and phenols [68,72] and out of plane deformation of C-H bonds in aromatic rings [72], respectively. In addition, according to other authors who characterized polyphenol-enriched extracts from other plant materials, such as Ilex paraguarensis [71], Rosmarinus officinalis [73], Garcinia mangostana [74] and grape seeds [75], the observed peaks at 1601, 1284 and 1036 cm−1 could be attributed to C=C ring stretching vibration [71,73,75], ester C-O stretching [75] or the presence of methoxy groups [74], and C-N stretching vibration of aliphatic amines [71], respectively. As a result of the aforementioned peak assignations, it was concluded that AVE contained a variety of phenolic compounds.

3.3.2. Thermogravimetric Analysis (TGA)

The thermal stability of AVE obtained under optimized MAE conditions was studied by thermogravimetric analysis. Figure 2b shows the TGA and DTGA of AVE obtained under an inert nitrogen atmosphere. The thermal degradation process occurred over a wide range of temperatures, showing multiple overlapped decomposition steps which are in accordance with the complex composition of AVE. Similar behavior was reported for the thermal degradation process of other natural extracts, such as those from cocoa shell bean [5], grape seed [75] and yerba mate [71]. According to Figure 2b, the initial step of weight loss started below 100 °C, and it could be associated with water and volatile phenolic compound desorption. The subsequent degradation stages with peaks shown at 215.0 ± 0.4, 301.6 ± 2.0 and 442.1 ± 1.3 °C were relatively overlapped, and they were attributed to the thermal degradation of groups of biomolecules with different structural features and characteristics present in AVE. The second degradation step occurred from 125 to 272 °C with an associated mass loss of 27.3%, and it could be related to the degradation of some low to mid molecular weight components of AVE, such as the compounds which will be further discussed in Section 3.3.3. The third and fourth thermal degradation stages extended from 272 to 400 °C and from 400 to 800 °C with mass losses of 17.3 and 14.7%, respectively. These degradation processes may be ascribed to compounds with higher molecular weights and more complex structures such as cellulose and lignin derivatives that might be present in Aloe vera extracts [70]. Finally, nearly 34.1 ± 0.1% of the initial weight remained at 800 °C as char residue, which could be related to non-pyrolyzable compounds.

3.3.3. Determination of Phenolic Profile by HPLC

Optimization of chromatographic conditions (flow rate, mobile phase composition and gradient step) was performed on AVE in order to obtain an adequate peak separation and resolution. Contrary to some authors who reported that a methanol–water mobile phase added with formic or acetic acid was suitable for phenolic profiling of different aloe species [76,77,78], in this study it was found that peak shape and separation efficiency of phenolic compounds in AVE were significantly improved by using an acetonitrile–water mixture, which was selected as the mobile phase in accordance with previous works [47,48,79]. Aloesin, chlorogenic acid, orientin, aloeresin D, aloin B, aloin A, cinnamic acid and aloe-emodin, whose chemical structures are shown in Figure 3, were identified in AVE obtained under optimal MAE conditions by HPLC-ESI-MS/MS by comparing their retention times and mass spectra with those of commercial standards. These results are in general agreement with previous works reporting the presence of these compounds in Aloe vera extracts [47,48,76]. It has been stated that the beneficial health-promoting properties found in Aloe leaves might be related to the highly complex phytochemical composition and, in particular, to characteristic phenolic compounds which could act against free radical and oxidative processes [80]. However, a general consensus on the role of some of these phenolic compounds has not been achieved yet, and some studies have highlighted their potential adverse effects [20].
Even though some authors have reported that Aloe contains many common phenolic acid derivatives (gallic acid, protocatechuic acid, syringic acid, gentisic acid), hydroxycinnamic acid derivatives (p-coumaric acid, ferulic acid, caffeic acid, sinapic acid) and flavonoids (naringenin, catechin, epicatechin, kaempferol, rutin, luteolin, myricetin) [4,42,81], only a fraction of the targeted standards was identified in AVE. This fact could be related to the influence of some environmental conditions, such as water and sunlight availability, soil characteristics (pH, conductivity, total N), geographical origin, plant variety and age, harvest season, position of the leaves in the plant and post-harvest treatment, among many other factors, which combined with the effect of the extraction technique could significantly affect secondary metabolite composition in plants [51,79,82]. In addition, it was noticed that m/z signals corresponding to several aforementioned compounds were recorded at different retention times compared to the standards, suggesting that isomeric compounds of target polyphenols might be present in AVE.
The phenolic compounds identified in AVE were quantified by HPLC-DAD (Figure 4a). Calibration curves of aloesin, chlorogenic acid, orientin, aloeresin D, aloin B, aloin A, cinnamic acid and aloe-emodin were obtained, showing acceptable levels of linearity with determination coefficients (R2) ranging from 0.9960 to 0.9999 for all the analyzed standards at ten concentration levels (Table 5). The LOD and LOQ values that were obtained ranged from 0.018 to 0.383 mg kg−1 and from 0.061 to 1.275 mg kg−1, respectively, indicating the feasibility of the proposed method for the quantification of the identified polyphenols. Finally, precision in terms of repeatability was evaluated by analyzing standard solutions, in triplicate, for all concentration levels within the same day, with relative standard deviations ranging from 0.9 to 2.6%, showing good repeatability. Diastereomeric anthraquinone derivatives Aloin A and B were the main components present in AVE, accounting for 702 ± 2 and 308.1 ± 0.6 mg 100 g AVS−1, respectively. Another major component found in AVE was the chromone aloesin with a concentration of 292.6 ± 0.5 mg 100 g AVS−1. Other quantified phenolic compounds ranged from 3.6 ± 0.1 to 80.0 ± 0.2 mg 100 g AVS−1. Quantification results and analytical figures of merit for HPLC-DAD analysis are summarized in Table 5.
Phenolic compounds present in Aloe vera plant have been extensively studied in recent decades due to their well-known beneficial and health promoting properties. However, the vast majority of the research was focused on the inner gel of the plant and very few reports on Aloe vera skin phenolic profiles and contents are currently available. Añibarro-Ortega et al. [13] reported that chromones and anthrones accounted for up to 44.9% and 43.8% of the phenolic compounds found in Aloe vera rind extract, respectively, with the concentration of aloesin, aloin B and aloin A being 34.4 ± 0.7, 4.3 ± 0.3 and 9.9 ± 0.4 mg g AVE−1, respectively. The relative concentration reported for aloin A and B diastereomers is in close agreement with the results shown in Table 5, and aloin A was 2.3 times more concentrated than aloin B, although smaller quantities of both aloins were reported. On the other hand, López et al. [42] found a lower chlorogenic acid concentration in AVS, accounting for only 7.8 ± 0.2 mg 100 g AVS−1. Lucini et al. [4] suggested that hydroxycinnamic acids, anthrones and chromones might have a direct and relevant role in the antioxidant potential of Aloe vera extracts.
Other studies reported quantitative contents of aloesin, aloeresin D, aloin A, aloin B, aloe-emodin, orientin, cinnamic acid and chlorogenic acid [76,78,83,84,85,86]. However, different plant species, Aloe plant tissues (i.e., whole leaf, gel, exudate) and processing and extraction techniques were used, and comparison of quantification results might not be straightforward. For instance, Lai et al. [83] reported 4.26 ± 0.14 and 25.81 ± 0.21 mg 100 g FW−1 of whole Aloe barbadensis leaf for chlorogenic acid and total aloin, respectively. Moreover, Cardarelli et al. [86] analyzed exudates from six-year-old Aloe barbadendis plants and found 2.81± 0.21, 0.042 ± 0.007, 0.016 ± 0.001, 1.96 ± 0.40 and 3.27 ± 0.20 100−1 g of aloin, aloe-emodin, aloenin, aloesin and aloeresin A, respectively. Similarly, Wu et al. [76] found that the main component present in Aloe barbadensis exudate was aloin A, accounting for 178 to 219 mg g−1. Moreover, aloesin and aloe-emodin contents ranged from 0.90 to 19.3 and from 0.96 to 2.27 mg g−1, respectively. On the other hand, Aldayel et al. [84] reported 43.3 ± 2.8 and 21.4 ± 2.0 mg g−1 of Aloe vera gel extract for aloin B and A, respectively. In conclusion, a wide range of quantitative results could be found in the literature using different approaches for the analysis of Aloe vera plant components.
Apart from the eight already quantified phenolic compounds, other peaks were also detected in the negative ion mode as [M-H],- and they were tentatively identified based on their accurate mass fragments, elution sequence and careful analysis of the literature (Table 6). A typical total ion chromatogram (TIC) of AVE obtained by HPLC-MS is shown in Figure 4b. The MS spectrum found for peak a showed the most abundant fragment at m/z 455. Añibarro-Ortega et al. [13] reported similar findings, although the structure of this compound has not yet been elucidated. Peak b eluted at 13.0 min, showing fragments at m/z 337 and 609, which were tentatively identified as cis or trans-5-p-coumaroylquinic acid and luteolin-6,8-C-diglucoside, respectively, by the same authors. The mass spectrum for peak c exhibited a main fragment at m/z 447, revealing a group of orientin isomers which, according to the literature, might be identified as 8-O-methyl-7-hydroxyaloin [47,84] or luteolin-6-C-glucoside [13]. Peaks d and e showed a main fragment at m/z 433. It has been reported that Aloe vera extracts contain aloin-derived diastereoisomers such as 5, 7 or 10-hydroxyaloin, which were proposed for the tentative identification of these peaks [13,47,48,76,85]. Similarly, peaks f, g, h and j were tentatively identified as dihydroisocoumarin glucoside [84], 6′-malonylnataloin B [47,48], 6′-malonylnataloin A [47,48] and 5,3′-dihydroxy-6,7,4′-trimethoxyflavone [48], respectively. Finally, peak i showed a main fragment at m/z 585. A compound with 585 g mol−1 of molecular weight was also found by Añibarro-Ortega et al. [13], although its molecular structure was not determined.
Table
Table 6. Tentative identification of unknown phenolic compounds in AVE by HPLC-MS.
Table 6. Tentative identification of unknown phenolic compounds in AVE by HPLC-MS.
Peak 1tR 2(m/z)Elemental
Composition		Tentative IdentificationRef.
(min)[M-H]-
a10.9455-Unknown[13]
b13337C16H17O8-cis or trans 5-p-Coumaroylquinic acid[13]
609C27H29O16-luteolin-6,8-C-diglucoside[13]
c13.8447C22H23O10-8-O-methyl-7-hydroxyaloin[47,84]
447C22H23O10-luteolin-6-C-glucoside[13]
d15.2433C21H21O10-7-hydroxyaloin B[47]
433C21H21O10-10-hydroxyaloin B[13,48,76,85]
433C21H21O10-5-hydroxyaloin B[13]
e15.9433C21H21O10-7-hydroxyaloin A[47]
433C21H21O10-10-hydroxyaloin A[13,48,76,85]
433C21H21O10-5-hydroxyaloin A[13]
f17.7505C24H25O12-Dihydroisocoumarin glucoside[84]
g20.2459C23H23O10-6′-malonylnataloin B[47,48]
h20.8459C23H23O10-6′-malonylnataloin A[47,48]
i24.2585-Unknown[13]
j24.7343C18H15O7-5,3′-Dihydroxy-6,7,4′-trimethoxyflavone[48]
1 Notation for peak identification refers to Figure 4. 2 Retention times from HPLC-MS according to extracted ion chromatograms (EICs).

3.4. Scanning Electron Microscopy (SEM)

SEM was used to investigate the impact of the MAE process on the AVS structure. Figure 5a,b show SEM micrographs obtained for raw AVS after drying and grinding steps as well as for AVS residue obtained after MAE under optimal conditions, respectively. A significant change in the surface morphology of the AVS particles was observed. Before extraction, particles exhibited a relatively smooth and unaltered surface. However, after MAE, AVS showed increased porosity and evidenced surface deterioration. These results are in accordance with other authors reporting similar effects of microwave irradiation on diverse vegetal materials such as cocoa bean shell [5], Pinus radiata bark [87] and brown seaweeds [88]. In all cases, it was suggested that the damage to the vegetal structure can facilitate solvent penetration, enhancing diffusion and extraction of bioactive compounds, which helps to increase TPC and antioxidant activity values.

4. Conclusions

A new MAE methodology was developed for the extraction of bioactive compounds from Aloe vera skin wastes as a green and fast strategy for the valorization of these agrowastes. The combined effects of MAE experimental parameters such as ethanol composition, temperature, time and solvent volume on extraction yield, TPC, DPPH, FRAP and aloin content of the extracts were studied and optimized by using a BBD. Second-order polynomial regression models with high reliability were obtained and MAE conditions which simultaneously optimize all responses were 80% ethanol, 80 °C, 36.6 min and 50.0 mL. Under these extraction conditions, the obtained responses regarding extraction yield, TPC, DPPH, FRAP and aloin were 17.3 ± 0.1 g AVE 100 g AVS−1, 116.4 ± 4.5 mg GAE g AVE−1, 69.0 ± 1.9 mg TE g AVE−1, 131.9 ± 6.5 mg TE g AVE−1 and 55.6 ± 0.2 mg aloin g AVE−1, respectively. Structural (FTIR) and thermal (TGA) characterization results were in accordance with AVE composition, while significant differences in surface morphology were evidenced by SEM in AVS before and after MAE. Moreover, eight major phenolic compounds (aloesin, chlorogenic acid, orientin, aloeresin D, aloin B, aloin A, cinnamic acid and aloe-emodin) were identified and quantified by HPLC-DAD/MS, while eight other compounds were also tentatively identified. Diastereomeric anthraquinone derivatives Aloin A and B were the main components present in AVE, followed by the chromone aloesin. According to the obtained results, the proposed method could be a promising procedure for obtaining antioxidant extracts rich in polyphenols with potential industrial applications in the food, biomedical or cosmeceutical industries, as well as contributing to the circular economy and reducing food waste and environmental impact issues.

Author Contributions

Conceptualization, A.J. and M.C.G.; methodology, A.J. and M.C.G.; validation, A.J. and M.C.G.; formal analysis, I.S.; investigation, I.S.; data curation, I.S.; writing—original draft preparation, I.S.; writing—review and editing, A.J. and M.C.G.; supervision, A.J. and M.C.G. All authors have read and agreed to the published version of the manuscript.

Funding

Authors would like to acknowledge Consellería de Educación, Investigación, Cultura y Deporte de la Generalitat Valenciana (GRISOLIAP/2016/081) and Spanish Ministry of Science and Innovation (Refs. PID2020-116496RB-C21, PDC2021-121345-C21) for their financial support.

Institutional Review Board Statement

Not applicable.

Informed Consent Statement

Not applicable.

Data Availability Statement

Data are contained within the article.

Acknowledgments

Authors acknowledge LAS CORONAS for providing Aloe vera leaves.

Conflicts of Interest

The authors declare no conflict of interest.

References

  1. Esposito, B.; Sessa, M.R.; Sica, D.; Malandrino, O. Towards Circular Economy in the Agri-Food Sector. A Systematic Literature Review. Sustainability 2020, 12, 7401. [Google Scholar] [CrossRef]
  2. Baiano, A. Recovery of Biomolecules from Food Wastes—A Review. Molecules 2014, 19, 14821–14842. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  3. Flores-López, M.L.; Romaní, A.; Cerqueira, M.A.; Rodríguez-García, R.; Jasso de Rodríguez, D.; Vicente, A.A. Compositional Features and Bioactive Properties of Whole Fraction from Aloe vera Processing. Ind. Crops Prod. 2016, 91, 179–185. [Google Scholar] [CrossRef] [Green Version]
  4. Lucini, L.; Pellizzoni, M.; Pellegrino, R.; Pietro Molinari, G.; Colla, G. Phytochemical Constituents and In Vitro Radical Scavenging Activity of Different Aloe Species. Food Chem. 2015, 170, 501–507. [Google Scholar] [CrossRef]
  5. Mellinas, A.C.; Jiménez, A.; Garrigós, M.C. Optimization of Microwave-Assisted Extraction of Cocoa Bean Shell Waste and Evaluation of Its Antioxidant, Physicochemical and Functional Properties. LWT 2020, 127, 109361. [Google Scholar] [CrossRef]
  6. Ninčević Grassino, A.; Djaković, S.; Bosiljkov, T.; Halambek, J.; Zorić, Z.; Dragović-Uzelac, V.; Petrović, M.; Rimac Brnčić, S. Valorisation of Tomato Peel Waste as a Sustainable Source for Pectin, Polyphenols and Fatty Acids Recovery Using Sequential Extraction. Waste Biomass Valori. 2020, 11, 4593–4611. [Google Scholar] [CrossRef]
  7. Quiles-Carrillo, L.; Mellinas, C.; Garrigos, M.C.; Balart, R.; Torres-Giner, S. Optimization of Microwave-Assisted Extraction of Phenolic Compounds with Antioxidant Activity from Carob Pods. Food Anal. Methods 2019, 12, 2480–2490. [Google Scholar] [CrossRef]
  8. Baruah, A.; Bordoloi, M.; Deka Baruah, H.P. Aloe vera: A Multipurpose Industrial Crop. Ind. Crops Prod. 2016, 94, 951–963. [Google Scholar] [CrossRef]
  9. Hęś, M.; Dziedzic, K.; Górecka, D.; Jędrusek-Golińska, A.; Gujska, E. Aloe vera (L.) Webb.: Natural Sources of Antioxidants—A Review. Plant Foods Hum. Nutr. 2019, 74, 255–265. [Google Scholar] [CrossRef] [Green Version]
  10. Rodríguez-Rodríguez, E.; Darias-Martín, J.; Díaz-Romero, C. Aloe vera as a Functional Ingredient in Foods. Crit. Rev. Food Sci. Nutr. 2010, 50, 305–326. [Google Scholar] [CrossRef]
  11. Eshun, K.; He, Q. Aloe vera: A Valuable Ingredient for the Food, Pharmaceutical and Cosmetic Industries—A Review. Crit. Rev. Food Sci. Nutr. 2004, 44, 91–96. [Google Scholar] [CrossRef] [PubMed]
  12. Rajeswari, G.; Arutselvy, B.; Jacob, S. Delignification of Aloe vera Rind by Mild Acid Associated Microwave Pretreatment to Persuade Enhanced Enzymatic Saccharification. Waste Biomass Valori. 2020, 11, 5965–5975. [Google Scholar] [CrossRef]
  13. Añibarro-Ortega, M.; Pinela, J.; Barros, L.; Ćirić, A.; Silva, S.P.; Coelho, E.; Mocan, A.; Calhelha, R.C.; Soković, M.; Coimbra, M.A.; et al. Compositional Features and Bioactive Properties of Aloe vera Leaf (Fillet, Mucilage, and Rind) and Flower. Antioxidants 2019, 8, 444. [Google Scholar] [CrossRef] [Green Version]
  14. Solaberrieta, I.; Jiménez, A.; Cacciotti, I.; Garrigós, M.C. Encapsulation of Bioactive Compounds from Aloe vera Agrowastes in Electrospun Poly (Ethylene Oxide) Nanofibers. Polymers 2020, 12, 1323. [Google Scholar] [CrossRef]
  15. Salehi, B.; Albayrak, S.; Antolak, H.; Kręgiel, D.; Pawlikowska, E.; Sharifi-Rad, M.; Uprety, Y.; Tsouh Fokou, P.; Yousef, Z.; Amiruddin Zakaria, Z.; et al. Aloe Genus Plants: From Farm to Food Applications and Phytopharmacotherapy. Int. J. Mol. Sci. 2018, 19, 2843. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  16. Ding, W.-J.; Wu, X.-F.; Zhong, J.-S.; Wan, J.-Z. Effects of Temperature, PH and Light on the Stability of Aloin A and Characterisation of Its Major Degradation Products. Int. J. Food Sci. Technol. 2014, 49, 1773–1779. [Google Scholar] [CrossRef]
  17. Duval, J.; Pecher, V.; Poujol, M.; Lesellier, E. Research Advances for the Extraction, Analysis and Uses of Anthraquinones: A Review. Ind. Crops Prod. 2016, 94, 812–833. [Google Scholar] [CrossRef]
  18. Pellizzoni, M.; Ruzickova, G.; Kalhotka, L.; Lucini, L. Antimicrobial Activity of Different Aloe barbadensis Mill. and Aloe arborescens Mill. Leaf Fractions. J. Med. Plant Res. 2012, 6, 1975–1981. [Google Scholar] [CrossRef]
  19. Lucini, L.; Pellizzoni, M.; Molinari, G. Pietro Anthraquinones and β-Polysaccharides Content and Distribution in Aloe Plants Grown under Different Light Intensities. Biochem. Syst. Ecol. 2013, 51, 264–268. [Google Scholar] [CrossRef]
  20. Guo, X.; Mei, N. Aloe vera: A Review of Toxicity and Adverse Clinical Effects. J. Environ. Sci. Health C Environ. Carcinog. Ecotoxicol. Rev. 2016, 34, 77–96. [Google Scholar] [CrossRef]
  21. Boudreau, M.D.; Beland, F.A. An Evaluation of the Biological and Toxicological Properties of Aloe barbadensis (Miller), Aloe vera. J. Environ. Sci. Health C Environ. Carcinog. Ecotoxicol. Rev. 2006, 24, 103–154. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  22. Zonta, F.; Bogoni, P.; Masotti, P.; Micali, G. High-Performance Liquid Chromatographic Profiles of Aloe Constituents and Determination of Aloin in Beverages, with Reference to the EEC Regulation for Flavouring Substances. J. Chromatogr. A 1995, 718, 99–106. [Google Scholar] [CrossRef]
  23. Azmir, J.; Zaidul, I.S.M.; Rahman, M.M.; Sharif, K.M.; Mohamed, A.; Sahena, F.; Jahurul, M.H.A.; Ghafoor, K.; Norulaini, N.A.N.; Omar, A.K.M. Techniques for Extraction of Bioactive Compounds from Plant Materials: A Review. J. Food Eng. 2013, 117, 426–436. [Google Scholar] [CrossRef]
  24. Garcia-Salas, P.; Morales-Soto, A.; Segura-Carretero, A.; Fernández-Gutiérrez, A. Phenolic-Compound-Extraction Systems for Fruit and Vegetable Samples. Molecules 2010, 15, 8813–8826. [Google Scholar] [CrossRef] [PubMed]
  25. Ameer, K.; Shahbaz, H.M.; Kwon, J.-H. Green Extraction Methods for Polyphenols from Plant Matrices and Their Byproducts: A Review. Compr. Rev. Food Sci. Food Saf. 2017, 16, 295–315. [Google Scholar] [CrossRef] [Green Version]
  26. Chan, C.-H.; Yusoff, R.; Ngoh, G.-C.; Kung, F.W.-L. Microwave-Assisted Extractions of Active Ingredients from Plants. J. Chromatogr. A 2011, 1218, 6213–6225. [Google Scholar] [CrossRef]
  27. Kala, H.K.; Mehta, R.; Sen, K.K.; Tandey, R.; Mandal, V. Critical Analysis of Research Trends and Issues in Microwave Assisted Extraction of Phenolics: Have We Really Done Enough. TrAC-Trends Anal. Chem. 2016, 85, 140–152. [Google Scholar] [CrossRef]
  28. Veggi, P.C.; Martínez, J.; Meireles, M.A.A. Fundamentals of Microwave Extraction. In Microwave-Assisted Extraction for Bioactive Compounds: Theory and Practice; Chemat, F., Cravotto, G., Eds.; Springer: New York, NY, USA, 2013; pp. 15–52. [Google Scholar]
  29. Kala, H.K.; Mehta, R.; Tandey, R.; Sen, K.K.; Mandal, V. Ten Years of Research on Phenolics (2005–2015): A Status Report. Pacific Sci. Rev. A Nat. Sci. Eng. 2016, 18, 1–4. [Google Scholar] [CrossRef] [Green Version]
  30. Khoddami, A.; Wilkes, M.; Roberts, T. Techniques for Analysis of Plant Phenolic Compounds. Molecules 2013, 18, 2328–2375. [Google Scholar] [CrossRef]
  31. Yang, M.; Sun, J.; Lu, Z.; Chen, G.; Guan, S.; Liu, X.; Jiang, B.; Ye, M.; Guo, D.A. Phytochemical Analysis of Traditional Chinese Medicine Using Liquid Chromatography Coupled with Mass Spectrometry. J. Chromatogr. A 2009, 1216, 2045–2062. [Google Scholar] [CrossRef]
  32. Zhao, C.-N.; Tang, G.-Y.; Cao, S.-Y.; Xu, X.-Y.; Gan, R.-Y.; Liu, Q.; Mao, Q.-Q.; Shang, A.; Li, H.-B. Phenolic Profiles and Antioxidant Activities of 30 Tea Infusions from Green, Black, Oolong, White, Yellow and Dark Teas. Antioxidants 2019, 8, 215. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  33. Li, Y.; Cao, S.-Y.; Lin, S.-J.; Zhang, J.-R.; Gan, R.-Y.; Li, H.-B. Polyphenolic Profile and Antioxidant Capacity of Extracts from Gordonia Axillaris Fruits. Antioxidants 2019, 8, 150. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  34. Masek, A.; Latos-Brozio, M.; Chrzescijanska, E.; Podsedek, A. Polyphenolic Profile and Antioxidant Activity of Juglans regia L. Leaves and Husk Extracts. Forests 2019, 10, 988. [Google Scholar] [CrossRef] [Green Version]
  35. Radojković, M.; Moreira, M.M.; Soares, C.; Fátima Barroso, M.; Cvetanović, A.; Švarc-Gajić, J.; Morais, S.; Delerue-Matos, C. Microwave-Assisted Extraction of Phenolic Compounds from Morus Nigra Leaves: Optimization and Characterization of the Antioxidant Activity and Phenolic Composition. J. Chem. Technol. Biotechnol. 2018, 93, 1684–1693. [Google Scholar] [CrossRef] [Green Version]
  36. Angiolillo, L.; Del Nobile, M.A.; Conte, A. The Extraction of Bioactive Compounds from Food Residues Using Microwaves. Curr. Opin. Food Sci. 2015, 5, 93–98. [Google Scholar] [CrossRef]
  37. Horwitz, W. (Ed.) Official Methods of Analysis of AOAC International, 17th ed.; Association of Official Analytical Chemists AOAC: Washington, DC, USA, 2000. [Google Scholar]
  38. Femenia, A.; Sánchez, E.S.; Simal, S.; Rosselló, C. Compositional Features of Polysaccharides from Aloe vera (Aloe barbadensis Miller) Plant Tissues. Carbohydr. Polym. 1999, 39, 109–117. [Google Scholar] [CrossRef]
  39. Pinela, J.; Prieto, M.A.; Carvalho, A.M.; Barreiro, M.F.; Oliveira, M.B.P.P.; Barros, L.; Ferreira, I.C.F.R. Microwave-Assisted Extraction of Phenolic Acids and Flavonoids and Production of Antioxidant Ingredients from Tomato: A Nutraceutical-Oriented Optimization Study. Sep. Purif. Technol. 2016, 164, 114–124. [Google Scholar] [CrossRef] [Green Version]
  40. Valdés, A.; Vidal, L.; Beltrán, A.; Canals, A.; Garrigós, M.C. Microwave-Assisted Extraction of Phenolic Compounds from Almond Skin Byproducts (Prunus amygdalus): A Multivariate Analysis Approach. J. Agric. Food Chem. 2015, 63, 5395–5402. [Google Scholar] [CrossRef] [Green Version]
  41. Prat, D.; Wells, A.; Hayler, J.; Sneddon, H.; McElroy, C.R.; Abou-Shehada, S.; Dunn, P.J. CHEM21 Selection Guide of Classical- and Less Classical-Solvents. Green Chem. 2016, 18, 288–296. [Google Scholar] [CrossRef] [Green Version]
  42. López, A.; Suárez de Tangil, M.; Vega-Orellana, O.; Ramírez, A.; Rico, M. Phenolic Constituents, Antioxidant and Preliminary Antimycoplasmic Activities of Leaf Skin and Flowers of Aloe vera (L.) Burm. f. (Syn. A. barbadensis Mill.) from the Canary Islands (Spain). Molecules 2013, 18, 4942–4954. [Google Scholar] [CrossRef] [Green Version]
  43. Kim, S.; Asnin, L.; Assefa, A.D.; Ko, E.Y.; Sharma, K.; Park, S.W. Extraction of Antioxidants from Aloe vera Leaf Gel: A Response Surface Methodology Study. Food Anal. Methods 2014, 7, 1804–1815. [Google Scholar] [CrossRef]
  44. Hu, Y.; Xu, J.; Hu, Q. Evaluation of Antioxidant Potential of Aloe vera (Aloe barbadensis Miller) Extracts. J. Agric. Food Chem. 2003, 51, 7788–7791. [Google Scholar] [CrossRef]
  45. Benzie, I.F.F.; Strain, J.J. The Ferric Reducing Ability of Plasma (FRAP) as a Measure of “Antioxidant Power”: The FRAP Assay. Anal. Biochem. 1996, 239, 70–76. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  46. Brown, P.N.; Yu, R.; Kuan, C.H.; Finley, J.; Mudge, E.M.; Dentali, S. Determination of Aloin A and Aloin B in Aloe vera Raw Materials and Finished Products by High-Performance Liquid Chromatography: Single-Laboratory Validation. J. AOAC Int. 2014, 97, 1323–1328. [Google Scholar] [CrossRef]
  47. Lee, S.; Do, S.-G.; Kim, S.Y.; Kim, J.; Jin, Y.; Lee, C.H. Mass Spectrometry-Based Metabolite Profiling and Antioxidant Activity of Aloe vera (Aloe barbadensis Miller) in Different Growth Stages. J. Agric. Food Chem. 2012, 60, 11222–11228. [Google Scholar] [CrossRef]
  48. Quispe, C.; Villalobos, M.; Bórquez, J.; Simirgiotis, M. Chemical Composition and Antioxidant Activity of Aloe vera from the Pica Oasis (Tarapacá, Chile) by UHPLC-Q/Orbitrap/MS/MS. J. Chem. 2018, 2018, 6123850. [Google Scholar] [CrossRef] [Green Version]
  49. Zapata, P.J.; Navarro, D.; Guillén, F.; Castillo, S.; Martínez-Romero, D.; Valero, D.; Serrano, M. Characterisation of Gels from Different Aloe Spp. as Antifungal Treatment: Potential Crops for Industrial Applications. Ind. Crops Prod. 2013, 42, 223–230. [Google Scholar] [CrossRef]
  50. Ray, A.; Gupta, S.D.; Ghosh, S. Evaluation of Anti-Oxidative Activity and UV Absorption Potential of the Extracts of Aloe vera L. Gel from Different Growth Periods of Plants. Ind. Crops Prod. 2013, 49, 712–719. [Google Scholar] [CrossRef]
  51. Kumar, S.; Yadav, M.; Yadav, A.; Yadav, J.P. Impact of Spatial and Climatic Conditions on Phytochemical Diversity and in Vitro Antioxidant Activity of Indian Aloe vera (L.) Burm.F. S. Afr. J. Bot. 2017, 111, 50–59. [Google Scholar] [CrossRef]
  52. Ng, Z.X.; Yong, P.H.; Lim, S.Y. Customized Drying Treatments Increased the Extraction of Phytochemicals and Antioxidant Activity from Economically Viable Medicinal Plants. Ind. Crops Prod. 2020, 155, 112815. [Google Scholar] [CrossRef]
  53. Shi, X.-D.; Nie, S.-P.; Yin, J.-Y.; Que, Z.-Q.; Zhang, L.-J.; Huang, X.-J. Polysaccharide from Leaf Skin of Aloe barbadensis Miller: Part I. Extraction, Fractionation, Physicochemical Properties and Structural Characterization. Food Hydrocoll. 2017, 73, 176–183. [Google Scholar] [CrossRef]
  54. Dahmoune, F.; Nayak, B.; Moussi, K.; Remini, H.; Madani, K. Optimization of Microwave-Assisted Extraction of Polyphenols from Myrtus communis L. Leaves. Food Chem. 2015, 166, 585–595. [Google Scholar] [CrossRef] [PubMed]
  55. Milutinović, M.; Radovanović, N.; Ćorović, M.; Šiler-Marinković, S.; Rajilić-Stojanović, M.; Dimitrijević-Branković, S. Optimisation of Microwave-Assisted Extraction Parameters for Antioxidants from Waste Achillea millefolium Dust. Ind. Crops Prod. 2015, 77, 333–341. [Google Scholar] [CrossRef]
  56. Lin, D.; Ma, Q.; Zhang, Y.; Peng, Z. Phenolic Compounds with Antioxidant Activity from Strawberry Leaves: A Study on Microwave-Assisted Extraction Optimization. Prep. Biochem. Biotechnol. 2020, 50, 874–882. [Google Scholar] [CrossRef] [PubMed]
  57. Djemaa-Landri, K.; Hamri-Zeghichi, S.; Valls, J.; Cluzet, S.; Tristan, R.; Boulahbal, N.; Kadri, N.; Madani, K. Phenolic Content and Antioxidant Activities of Vitis Vinifera L. Leaf Extracts Obtained by Conventional Solvent and Microwave-Assisted Extractions. J. Food Meas. Charact. 2020, 14, 3551–3564. [Google Scholar] [CrossRef]
  58. Rudić, S.; Dimitrijević-Branković, S.; Dimitrijević, S.; Milić, M. Valorization of Unexploited Artichoke Leaves Dust for Obtaining of Extracts Rich in Natural Antioxidants. Sep. Purif. Technol. 2021, 256, 117714. [Google Scholar] [CrossRef]
  59. Chang, X.L.; Chen, B.Y.; Feng, Y.M. Water-Soluble Polysaccharides Isolated from Skin Juice, Gel Juice and Flower of Aloe vera Miller. J. Taiwan Inst. Chem. Eng. 2011, 42, 197–203. [Google Scholar] [CrossRef]
  60. Sultana, B.; Anwar, F.; Ashraf, M. Effect of Extraction Solvent/Technique on the Antioxidant Activity of Selected Medicinal Plant Extracts. Molecules 2009, 14, 2167–2180. [Google Scholar] [CrossRef]
  61. Ma, Y.; Li, J.; Tong, F.; Xin, X.-L.; Aisa, H.A. Optimization of Microwave-Assisted Extraction Using Response Surface Methodology and the Potential Anti-Diabetic Efficacy of Nigella glandulifera Freyn Determined Using the Spectrum–Effect Relationship. Ind. Crops Prod. 2020, 153, 112592. [Google Scholar] [CrossRef]
  62. Alara, O.R.; Abdurahman, N.H.; Ukaegbu, C.I.; Azhari, N.H. Vernonia cinerea Leaves as the Source of Phenolic Compounds, Antioxidants, and Anti-Diabetic Activity Using Microwave-Assisted Extraction Technique. Ind. Crops Prod. 2018, 122, 533–544. [Google Scholar] [CrossRef]
  63. Shahidi, F.; Ambigaipalan, P. Phenolics and Polyphenolics in Foods, Beverages and Spices: Antioxidant Activity and Health Effects—A Review. J. Funct. Foods 2015, 18, 820–897. [Google Scholar] [CrossRef]
  64. Liazid, A.; Palma, M.; Brigui, J.; Barroso, C.G. Investigation on Phenolic Compounds Stability during Microwave-Assisted Extraction. J. Chromatogr. A 2007, 1140, 29–34. [Google Scholar] [CrossRef] [PubMed]
  65. Gulcin, İ. Antioxidants and Antioxidant Methods: An Updated Overview. Arch. Toxicol. 2020, 94, 651–715. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  66. Milutinović, M.; Radovanović, N.; Rajilić-Stojanović, M.; Šiler-Marinković, S.; Dimitrijević, S.; Dimitrijević-Branković, S. Microwave-Assisted Extraction for the Recovery of Antioxidants from Waste Equisetum Arvense. Ind. Crops Prod. 2014, 61, 388–397. [Google Scholar] [CrossRef]
  67. Tian, B.; Hua, Y. Concentration-Dependence of Prooxidant and Antioxidant Effects of Aloin and Aloe-Emodin on DNA. Food Chem. 2005, 91, 413–418. [Google Scholar] [CrossRef]
  68. Sánchez, J.T.; García, A.V.; Martínez-Abad, A.; Vilaplana, F.; Jiménez, A.; Garrigós, M.C. Physicochemical and Functional Properties of Active Fish Gelatin-Based Edible Films Added with Aloe vera Gel. Foods 2020, 9, 1248. [Google Scholar] [CrossRef]
  69. Akbari, S.; Abdurahman, N.H.; Yunus, R.M.; Alsaggaf, A.H.A.; Ahmed, N. LC-QTOF-MS Analysis of Phenolics and Saponins Extracted from Aloe vera Leaves via Microwave Technology in Optimal Condition. S. Afr. J. Bot. 2021, 139, 362–373. [Google Scholar] [CrossRef]
  70. Barbosa, R.; Villarreal, A.; Rodriguez, C.; De Leon, H.; Gilkerson, R.; Lozano, K. Aloe vera Extract-Based Composite Nanofibers for Wound Dressing Applications. Mater. Sci. Eng. C 2021, 124, 112061. [Google Scholar] [CrossRef]
  71. Gullón, B.; Eibes, G.; Moreira, M.T.; Herrera, R.; Labidi, J.; Gullón, P. Yerba Mate Waste: A Sustainable Resource of Antioxidant Compounds. Ind. Crops Prod. 2018, 113, 398–405. [Google Scholar] [CrossRef]
  72. Jithendra, P.; Rajam, A.M.; Kalaivani, T.; Mandal, A.B.; Rose, C. Preparation and Characterization of Aloe vera Blended Collagen-Chitosan Composite Scaffold for Tissue Engineering Applications. ACS Appl. Mater. Inter. 2013, 5, 7291–7298. [Google Scholar] [CrossRef]
  73. Estevez-Areco, S.; Guz, L.; Candal, R.; Goyanes, S. Release Kinetics of Rosemary (Rosmarinus officinalis) Polyphenols from Polyvinyl Alcohol (PVA) Electrospun Nanofibers in Several Food Simulants. Food Packag. Shelf Life 2018, 18, 42–50. [Google Scholar] [CrossRef]
  74. Charernsriwilaiwat, N.; Rojanarata, T.; Ngawhirunpat, T.; Sukma, M.; Opanasopit, P. Electrospun Chitosan-Based Nanofiber Mats Loaded with Garcinia Mangostana Extracts. Int. J. Pharm. 2013, 452, 333–343. [Google Scholar] [CrossRef] [PubMed]
  75. Locilento, D.A.; Mercante, L.A.; Andre, R.S.; Mattoso, L.H.C.; Luna, G.L.F.; Brassolatti, P.; Anibal, F.d.F.; Correa, D.S. Biocompatible and Biodegradable Electrospun Nanofibrous Membranes Loaded with Grape Seed Extract for Wound Dressing Application. J. Nanomater. 2019, 2019, 2472964. [Google Scholar] [CrossRef] [Green Version]
  76. Wu, X.; Ding, W.; Zhong, J.; Wan, J.; Xie, Z. Simultaneous Qualitative and Quantitative Determination of Phenolic Compounds in Aloe Barbadensis Mill by Liquid Chromatography–Mass Spectrometry-Ion Trap-Time-of-Flight and High Performance Liquid Chromatography-Diode Array Detector. J. Pharm. Biomed. Anal. 2013, 80, 94–106. [Google Scholar] [CrossRef] [PubMed]
  77. Zhao, Y.; Sun, Y.N.; Lee, M.J.; Kim, Y.H.; Lee, W.; Kim, K.H.; Kim, K.T.; Kang, J.S. Identification and Discrimination of Three Common Aloe Species by High Performance Liquid Chromatography–Tandem Mass Spectrometry Coupled with Multivariate Analysis. J. Chromatogr. B 2016, 1031, 163–171. [Google Scholar] [CrossRef] [PubMed]
  78. Park, M.K.; Park, J.H.; Kim, N.Y.; Shin, Y.G.; Choi, Y.S.; Gyun, J.; Kim, K.H.; Lee, S.K. Analysis of 13 Phenolic Compounds in Aloe Species by High Performance Liquid Chromatography. Phytochem. Anal. 1998, 9, 186–191. [Google Scholar] [CrossRef]
  79. Kanama, S.K.; Viljoen, A.M.; Kamatou, G.P.P.P.; Chen, W.; Sandasi, M.; Adhami, H.R.; Van Wyk, B.E. Simultaneous Quantification of Anthrones and Chromones in Aloe Ferox (“Cape Aloes”) Using UHPLC-MS. Phytochem. Lett. 2015, 13, 85–90. [Google Scholar] [CrossRef]
  80. Loots, D.T.; van der Westhuizen, F.H.; Botes, L. Aloe Ferox Leaf Gel Phytochemical Content, Antioxidant Capacity, and Possible Health Benefits. J. Agric. Food Chem. 2007, 55, 6891–6896. [Google Scholar] [CrossRef]
  81. Debnath, T.; Ghosh, M.; Lee, Y.M.; Nath, N.C.D.; Lee, K.-G.; Lim, B.O. Identification of Phenolic Constituents and Antioxidant Activity of Aloe barbadensis Flower Extracts. Food Agric. Immunol. 2018, 29, 27–38. [Google Scholar] [CrossRef] [Green Version]
  82. Figueiredo, A.C.; Barroso, J.G.; Pedro, L.G.; Scheffer, J.J.C. Factors Affecting Secondary Metabolite Production in Plants: Volatile Components and Essential Oils. Flavour Fragr. J. 2008, 23, 213–226. [Google Scholar] [CrossRef]
  83. Lai, Q.; Wang, H.; Guo, X.; Abbasi, A.M.; Wang, T.; Li, T.; Fu, X.; Li, J.; Liu, R.H. Comparison of Phytochemical Profiles, Antioxidant and Cellular Antioxidant Activities of Seven Cultivars of Aloe. Int. J. Food Sci. Technol. 2016, 51, 1489–1494. [Google Scholar] [CrossRef]
  84. Aldayel, T.S.; Grace, M.H.; Lila, M.A.; Yahya, M.A.; Omar, U.M.; Alshammary, G. LC-MS Characterization of Bioactive Metabolites from Two Yemeni Aloe Spp. with Antioxidant and Antidiabetic Properties. Arab. J. Chem. 2020, 13, 5040–5049. [Google Scholar] [CrossRef]
  85. Zhong, J.-S.; Wan, J.-Z.; Ding, W.-J.; Wu, X.-F.; Xie, Z.-Y. Multi-Responses Extraction Optimization Combined with High-Performance Liquid Chromatography-Diode Array Detection–Electrospray Ionization-Tandem Mass Spectrometry and Chemometrics Techniques for the Fingerprint Analysis of Aloe barbadensis Miller. J. Pharm. Biomed. Anal. 2015, 107, 131–140. [Google Scholar] [CrossRef] [PubMed]
  86. Cardarelli, M.; Rouphael, Y.; Pellizzoni, M.; Colla, G.; Lucini, L. Profile of Bioactive Secondary Metabolites and Antioxidant Capacity of Leaf Exudates from Eighteen Aloe Species. Ind. Crops Prod. 2017, 108, 44–51. [Google Scholar] [CrossRef]
  87. Aspé, E.; Fernández, K. The Effect of Different Extraction Techniques on Extraction Yield, Total Phenolic, and Anti-Radical Capacity of Extracts from Pinus radiata Bark. Ind. Crops Prod. 2011, 34, 838–844. [Google Scholar] [CrossRef]
  88. Ummat, V.; Tiwari, B.K.; Jaiswal, A.K.; Condon, K.; Garcia-Vaquero, M.; O’Doherty, J.; O’Donnell, C.; Rajauria, G. Optimisation of Ultrasound Frequency, Extraction Time and Solvent for the Recovery of Polyphenols, Phlorotannins and Associated Antioxidant Activity from Brown Seaweeds. Mar. Drugs 2020, 18, 250. [Google Scholar] [CrossRef]
Antioxidants 11 01058 g001a 550Antioxidants 11 01058 g001b 550
Figure 1. Response surface plots of significant interactions between independent variables on: (a) TPC (volume vs. time); (b) DPPH (temperature vs. time); (c) FRAP (ethanol concentration vs. time) and (d) FRAP (ethanol concentration vs. solvent volume). In all cases, the other factors were fixed at their central values.
Figure 1. Response surface plots of significant interactions between independent variables on: (a) TPC (volume vs. time); (b) DPPH (temperature vs. time); (c) FRAP (ethanol concentration vs. time) and (d) FRAP (ethanol concentration vs. solvent volume). In all cases, the other factors were fixed at their central values.
Antioxidants 11 01058 g001aAntioxidants 11 01058 g001b
Antioxidants 11 01058 g002 550
Figure 2. FTIR spectrum (a) and TGA and DTGA thermograms (b) of AVE obtained under optimal MAE conditions.
Figure 2. FTIR spectrum (a) and TGA and DTGA thermograms (b) of AVE obtained under optimal MAE conditions.
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Antioxidants 11 01058 g003 550
Figure 3. Chemical structures of eight identified compounds by HPLC-MS in AVE. (1) aloesin; (2) chlorogenic acid; (3) orientin; (4) aloeresin D; (5) aloin B; (6) aloin A; (7) cinnamic acid; (8) aloe emodin.
Figure 3. Chemical structures of eight identified compounds by HPLC-MS in AVE. (1) aloesin; (2) chlorogenic acid; (3) orientin; (4) aloeresin D; (5) aloin B; (6) aloin A; (7) cinnamic acid; (8) aloe emodin.
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Antioxidants 11 01058 g004 550
Figure 4. (a) HPLC-DAD chromatogram showing the phenolic profile of AVE obtained under optimum MAE conditions; (b) HPLC-MS total ion chromatogram (TIC) of AVE. See Table 5; Table 6 for peak assignations.
Figure 4. (a) HPLC-DAD chromatogram showing the phenolic profile of AVE obtained under optimum MAE conditions; (b) HPLC-MS total ion chromatogram (TIC) of AVE. See Table 5; Table 6 for peak assignations.
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Antioxidants 11 01058 g005 550
Figure 5. SEM micrographs of raw AVS (a) and AVS after MAE under optimal conditions (b).
Figure 5. SEM micrographs of raw AVS (a) and AVS after MAE under optimal conditions (b).
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Table
Table 1. Leaf dimensions, Aloe vera waste yield and chemical characterization of Aloe vera skin (AVS). Results are expressed as mean ± SD.
Table 1. Leaf dimensions, Aloe vera waste yield and chemical characterization of Aloe vera skin (AVS). Results are expressed as mean ± SD.
Leaf Dimensions 1
Length (cm)64.9 ± 3.7
Width at base (cm)12.8 ± 0.8
Thickness (cm)2.8 ± 0.3
Waste yield 1,2
Weight (g)780 ± 90
Skin waste (%)15.1 ± 2.1
Chemical characterization of AVS 3
Moisture (g 100 g FW−1)84.9 ± 0.8
Ash (g 100 g DW−1)15.5 ± 0.1
Protein (g 100 g DW−1)6.5 ± 0.2
Lipids (g 100 g DW−1)2.4 ± 0.1
1n = 100; 2 Expressed as a fraction of the total leaf weight; 3 n = 3. FW: fresh weight; DW: dry weight.
Table
Table 2. Box-Behnken experimental design matrix and response values obtained from Aloe vera skin extracts using microwave-assisted extraction (MAE).
Table 2. Box-Behnken experimental design matrix and response values obtained from Aloe vera skin extracts using microwave-assisted extraction (MAE).
Experimental DomainResponse Variables
RunEt
(%, v/v)		T
(°C)		t
(min)		V
(mL)		Yield
(gAVE 100 gAVS−1)		TPC
(mgGAE gAVE−1)		DPPH
(mgTE gAVE−1)		FRAP
(mgTE gAVE−1)		Aloin
(mg gAVE−1)
1608022.58024.2104.9 ± 1.859.6 ± 5.1110.7 ± 3.246.1 ± 0.2
240605.06524.386.5 ± 0.951.4 ± 6.195.2 ± 3.739.2 ± 0.2
3608022.55018.8102.8 ± 1.465.0 ± 6.3120.2 ± 4.250.3 ± 0.1
4806022.55018.4122.4 ± 1.268.4 ± 5.3119.3 ± 3.253.0 ± 0.3
5406022.55022.991.1 ± 0.453.5 ± 6.2101.7 ± 1.742.0 ± 0.1
6606040.05022.5102.4 ± 0.558.7 ± 4.9109.9 ± 3.842.7 ± 0.2
7408022.56525.491.0 ± 0.961.6 ± 5.293.0 ± 2.039.0 ± 0.2
8604022.55021.1101.3 ± 0.554.9 ± 5.9116.2 ± 3.548.2 ± 0.3
9806022.58018.2121.3 ± 1.761.6 ± 4.5132.1 ± 0.754.2 ± 0.3
10806040.06518.7114.9 ± 1.659.3 ± 5.0130.7 ± 3.656.6 ± 0.5
11606022.56524.2105.4 ± 1.158.3 ± 4.2110.5 ± 5.746.9 ± 0.4
12604040.06523.2103.6 ± 1.054.4 ± 6.5108.7 ± 4.244.5 ± 0.3
13606022.56523.3102.2 ± 1.157.8 ± 2.1113.8 ± 3.046.1 ± 0.0
1460605.08023.998.5 ± 1.155.2 ± 5.5113.6 ± 3.945.4 ± 0.2
15804022.56518.8121.4 ± 1.168.1 ± 5.1134.1 ± 2.857.5 ± 0.2
16606022.56523.6104.0 ± 1.355.2 ± 4.9113.3 ± 4.347.1 ± 0.4
1780605.06520.3117.9 ± 1.264.3 ± 4.3116.3 ± 5.152.9 ± 0.1
18608040.06522.7103.6 ± 1.462.5 ± 4.4118.8 ± 1.947.1 ± 0.1
19808022.56519.4125.8 ± 1.373.4 ± 4.6131.5 ± 6.053.3 ± 0.3
20406040.06525.189.3 ± 0.449.9 ± 5.490.5 ± 2.436.5 ± 0.1
21406022.58026.387.4 ± 0.750.5 ± 5.699.6 ± 2.541.0 ± 0.1
2260605.05021.0116.3 ± 2.262.1 ± 2.9110.4 ± 1.844.8 ± 0.4
23606022.56524.7106.4 ± 0.958.8 ± 6.1108.2 ± 1.043.5 ± 0.2
24604022.58023.4102.7 ± 2.453.5 ± 6.2114.6 ± 5.447.6 ± 0.5
25606022.56524.9108.7 ± 2.359.1 ± 4.7109.6 ± 9.543.0 ± 0.3
2660405.06522.1109.4 ± 1.261.2 ± 7.0109.3 ± 0.245.6 ± 0.3
27404022.56524.888.8 ± 0.353.9 ± 6.297.7 ± 3.838.4 ± 0.3
28606040.08023.899.1 ± 0.654.1 ± 4.2119.7 ± 14.144.3 ± 0.1
2960805.06522.896.8 ± 1.253.4 ± 5.8106.3 ± 3.544.4 ± 0.4
Et: ethanol concentration; T: extraction temperature; t: extraction time; V: solvent volume. AVS: Aloe vera skin; AVE: Aloe vera extract; GAE: gallic acid equivalents; TE: trolox equivalents.
Table
Table 3. ANOVA results for response surface quadratic models of AVS extraction.
Table 3. ANOVA results for response surface quadratic models of AVS extraction.
SourceSum of SquaresDfMean SquareF-Valuep-Value
Yield
A102.081102.08215.820.0001 *
B0.0010.000.000.9685
C0.2110.210.450.5386
D19.00119.0040.170.0032 *
AA13.00113.0027.490.0063 *
AB0.0010.000.001.0000
AC1.4411.443.040.1560
AD3.2413.246.850.0590
BB5.2915.2911.190.0287 *
BC0.3610.360.760.4322
BD2.4012.405.080.0873
CC1.2611.262.670.1779
CD0.6410.641.350.3094
DD9.0119.0119.040.0120 *
Lack-of-fit6.02100.601.270.4399
Pure error1.8940.47
Total (corr.)157.5528
R20.9498
Adj R20.8995
TPC
A2995.6812995.68497.790.0000 *
B0.4410.440.070.8001
C13.02113.022.160.2153
D41.81141.816.950.0578
AA1.1511.150.190.6842
AB1.2111.210.200.6771
AC8.4118.411.400.3026
AD1.6911.690.280.6242
BB0.5510.550.090.7777
BC39.69139.696.600.0621
BD0.1210.120.020.8934
CC26.36126.364.380.1045
CD52.56152.568.730.0417 *
DD1.8111.810.300.6125
Lack-of-fit212.621021.263.530.1176
Pure error24.0746.02
Total (corr.)3422.5528
R20.9308
Adj R20.8617
DPPH
A460.041460.04189.860.0002 *
B72.52172.5229.930.0054 *
C6.3116.312.600.1819
D65.80165.8027.160.0065 *
AA20.94120.948.640.0424 *
AB1.4411.440.590.4838
AC3.0613.061.260.3238
AD3.6113.611.490.2893
BB40.43140.4316.690.0150 *
BC63.20163.2026.080.0069 *
BD4.0014.001.650.2682
CC22.88122.889.440.0372 *
CD1.3211.320.550.5010
DD1.9911.990.820.4165
Lack-of-fit108.491010.854.480.0808
Pure error9.6942.42
Total (corr.)902.5128
R20.8691
Adj R20.7381
FRAP
A2892.3112892.31499.790.0000 *
B0.0010.000.000.9910
C61.65161.6510.650.0310 *
D13.23113.232.290.2051
AA0.7110.710.120.7432
AB1.1011.100.190.6850
AC91.20191.2015.760.0165 *
AD55.50155.509.590.0363 *
BB28.42128.424.910.0910
BC42.90142.907.410.0528
BD15.60115.602.700.1759
CC22.66122.663.920.1189
CD10.89110.891.880.2420
DD56.67156.679.790.0352 *
Lack-of-fit214.981021.503.710.1088
Pure error23.1545.79
Total (corr.)3548.4728
R20.9329
Adj R20.8658
aloin
A696.161696.16186.040.0002 *
B0.2110.210.060.8230
C0.0310.030.010.9330
D0.4810.480.130.7383
AA11.79111.793.150.1505
AB5.7615.761.540.2825
AC10.24110.242.740.1734
AD1.2111.210.320.6000
BB8.5518.552.290.2051
BC3.6113.610.960.3816
BD3.2413.240.870.4048
CC7.8717.872.100.2205
CD0.2510.250.070.8088
DD4.6714.671.250.3266
Lack-of-fit37.29103.731.000.5501
Pure error14.9743.74
Total (corr.)809.1528
R20.9354
Adj R20.8708
A: ethanol concentration; B: extraction temperature; C: extraction time; D: solvent volume. * significant effect at p < 0.05.
Table
Table 4. Single response optimized extraction conditions and predicted values.
Table 4. Single response optimized extraction conditions and predicted values.
ResponseEt (%)T (°C)t (min)V (mL)Predicted Value
Yield40.067.726.780.026.8 g AVE 100 g AVS−1
TPC80.040.05.056.0127.4 mg GAE g AVE−1
DPPH80.080.040.052.773.4 mg TE gAVE−1
FRAP80.054.439.980.0140.5 mg TE gAVE−1
aloinMAX80.040.029.480.059.0 mg gAVE−1
aloinMIN40.040.340.061.835.4 mg gAVE−1
Et: ethanol concentration; T: extraction temperature; t: extraction time; V: solvent volume.
Table
Table 5. Phenolic compounds identified in AVE by HPLC-MS, analytical figures of merit and quantification results by HPLC-DAD.
Table 5. Phenolic compounds identified in AVE by HPLC-MS, analytical figures of merit and quantification results by HPLC-DAD.
Peak 1Compound(m/z) [M-H]-tR
(min)		Calibration Range
(mg kg−1)		Linearity
(R2)		LOD
(mg kg−1)		LOQ
(mg kg−1)		RSD 2
(%)		AVE
(mg 100 gAVS−1)
1aloesin3939.30.06–61.800.99980.1640.5462.6292.6 ± 0.5
2chlorogenic acid35310.50.05–99.700.99600.2130.7111.380.0 ± 0.2
3orientin44714.40.01–11.200.99910.0610.2032.346.5 ± 0.1
4aloeresin D55519.10.05–9.820.99710.3831.2752.639.7 ± 1.1
5aloin B41719.20.10–100.600.99980.0870.2921.1308.1 ± 0.6
6aloin A41720.00.20–202.100.99990.2780.9260.9702.0 ± 2.0
7cinnamic acid14725.20.004–3.7000.99920.0290.0951.413.6 ± 0.5
8aloe emodin26929.40.001–0.9000.99610.0180.0611.83.6 ± 0.1
1 peak assignation corresponding to Figure 4. 2 within-day precision (n = 3 at all concentration levels used in the calibration range).
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Solaberrieta, I.; Jiménez, A.; Garrigós, M.C. Valorization of Aloe vera Skin By-Products to Obtain Bioactive Compounds by Microwave-Assisted Extraction: Antioxidant Activity and Chemical Composition. Antioxidants 2022, 11, 1058. https://doi.org/10.3390/antiox11061058

AMA Style

Solaberrieta I, Jiménez A, Garrigós MC. Valorization of Aloe vera Skin By-Products to Obtain Bioactive Compounds by Microwave-Assisted Extraction: Antioxidant Activity and Chemical Composition. Antioxidants. 2022; 11(6):1058. https://doi.org/10.3390/antiox11061058

Chicago/Turabian Style

Solaberrieta, Ignacio, Alfonso Jiménez, and María Carmen Garrigós. 2022. "Valorization of Aloe vera Skin By-Products to Obtain Bioactive Compounds by Microwave-Assisted Extraction: Antioxidant Activity and Chemical Composition" Antioxidants 11, no. 6: 1058. https://doi.org/10.3390/antiox11061058

APA Style

Solaberrieta, I., Jiménez, A., & Garrigós, M. C. (2022). Valorization of Aloe vera Skin By-Products to Obtain Bioactive Compounds by Microwave-Assisted Extraction: Antioxidant Activity and Chemical Composition. Antioxidants, 11(6), 1058. https://doi.org/10.3390/antiox11061058

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