1. Introduction
Natural products (NPs) are natural compounds or substances produced by a living organism, which are found in nature. Owing to their structural diversity, they represent a relevant source of lead compounds [
1] suitable for the development of new drugs. Many NPs present structural similarities with certain endogenous compounds [
2]. These similarities confer on them the ability to interact with certain body receptors and trigger their intrinsic activity, which results in a therapeutic effect on living organisms. These natural products can be isolated from different sources, where marine [
3], animal [
4], microbial [
5] and vegetal [
6,
7] are some of the most representative ones, while the latter is the most frequently investigated nowadays.
The most common method to search for bioactive compounds consists of screening different sources that have previously demonstrated to have a considerable therapeutic potential [
8]. As mentioned above, vegetal sources have been widely investigated, which has led to the discovery of an extensive variety of compounds with pharmacological activity and potential against certain health disorders.
Moringa oleifera Lam. is a native tree from north India [
9]. It is commonly known as the miracle tree [
10], and it is traditionally known to have a substantial medicinal potential. Its leaves, pods and flowers have been extensively used for the treatment of certain metabolic disorders such as hypercholesterolemia [
10] or diabetes [
11]. Its bioactivity is fundamentally attributed to the presence of an enormous variety of NPs in its leaves, flowers and roots (proteins, vitamins, glucosinolates, alkaloids, flavonoids, phenolic compounds…) [
9,
10,
12] that confer this plant with its therapeutic potential as an antioxidant [
13], anti-inflammatory [
10,
14], anti-hyperlypidemic [
10] and hypoglycemic [
11] agent. All the abovementioned properties make
M. oleifera a good candidate to have its different parts screened in search of NPs that may have a therapeutical application regarding the treatment of a series of health disorders.
Phenolic compounds are common vegetal bioactive compounds, mainly known because of their antioxidant properties that make them suitable for the prevention of certain health issues related to oxidative processes, such as cancer or cardiovascular diseases [
15]. In fact,
M. oleifera is known to produce a large diversity of phenolic compounds (myricetin, quercetin and kaempferol derivatives, gallic and chlorogenic acid…) [
16,
17] that can be classified as flavonoid (anthocyanins, flavones, flavanones, flavanols, lignans…) [
18] or non-flavonoid compounds (phenolic acids and non-carboxylic phenols) [
19]. Flavonoids have been largely confirmed to act as antioxidant agents, as they can donate electrons to free radicals, which block the deleterious chain reactions involved in some degenerative processes, such as inflammation, diabetes or certain cardiovascular diseases [
20,
21]. Therefore, flavonoid-rich vegetal products, such as green tea [
22] or wine [
21], present potent antioxidant properties. Given the abundance of flavonoids in moringa plants, they are to be considered a great source of antioxidant compounds, where quercetin, kaempferol and their derivatives (quercetin 3-
O-rhamnoside, kaempferol glucosides…) are the most representative ones [
16,
23,
24].
Previous studies have been performed in this field, obtaining moringa extracts with phenolic contents of 20.16 mg gallic acid equivalents per gram of sample (GAE/g) [
25] or with a total phenolic content between 23.22 ± 1.12 and 43.96 ± 1.90 mg/g [
26] by using non-conventional extraction techniques, such as microwave-assisted extraction (MAE) or optimized ultrasound-assisted extraction (UAE).
The composition of the moringa extracts depends to a large extent on the plant tissue used as a sample, the extraction method and the specific extraction conditions [
27]. For that reason, before proceeding to any massive extractions, the design and optimization of an appropriate extraction method as well as the evaluation of the composition of the different sample sources (roots, flowers, leaves…) must be carried out. In this regard, enzymatic extraction (EE) has proven to be one of the most effective methods for the extraction of bioactive compounds, as it employs enzymes that catalytically break the plant cell walls and membranes, thus releasing all the compounds that are present in the cells into the solvent [
28]. When compared against other extraction techniques, such as ultrasound assisted extraction (UAE) or microwave assisted extraction (MAE), it can be seen that EE presents several advantages that support its position as the most suitable extraction method for this purpose. These advantages include scalability, high extraction yields [
29] and the fact that it can be implemented under mild conditions, which contributes to preserving the structural integrity of the bioactive compounds of interest [
28]. Furthermore, EE can be complemented with other techniques, such as UAE [
30]. Cellulases and pectinases are some of the enzymes most frequently used in EE, as cellulose and pectin are the most representative components in vegetal cell walls [
31,
32]. Apart from the type and amount of enzyme employed, other factors, such as the pH of the solvent and its composition, the temperature, agitation and the sample-to-solvent ratio as well as the extraction time [
33], are also variables to be taken into account for an optimal design of the extraction procedure.
Considering all of the factors mentioned above, the present study intends to develop an efficient EE method for obtaining the bioactive extracts that can be found in
M. oleifera and to demonstrate the antioxidant power of such extracts based on a number of chemical assays. The novelty of this study lies in the fact that a higher number of factors than usual is initially considered for the statistical design, which combines a screening Plackett–Burman design for the determination of the factors with a higher significance and a surface-response Box–Behnken design for their optimization [
34,
35]. It also intends to employ a greener technique (EE) than those used for conventional extraction methods (UAE, MAE) as it employs lower temperatures, lower amounts of organic solvents and requires less extraction times for the obtention of the extracts.
2. Materials and Methods
2.1. Plant Material
Dried leaves of M. oleifera were provided by the company Connatur (36.334872, −6.111330; Conil, Spain), which specialises in the cultivation and commercialisation of moringa. The dried leaves were ground in a conventional mill and sieved to a pore size of 200 mesh.
2.2. Solvents and Reagents
The extraction solvents consisted of variable percentages of absolute ethanol EssentQ® (Scharlab, Barcelona, Spain) diluted in different citrate/phosphate buffers at pH 4.0, 5.0 and 6.0 obtained by solving calcium citrate (Panreac S.L.U., Castellar del Vallés, Spain) and sodium dihydrogenphosphate (Panreac S.L.U., Castellar del Vallés, Spain) in Milli-Q water obtained by filtration through a MilliPore system (Bedford, MA, USA). The enzyme employed for the extraction was a pectinase obtained from Aspergillus niger (Merck KgaA, Darmstadt, Germany).
For the determination of the antioxidant capacity of the extract, 2,2-diphenyl-1-picrylhydrazyl (DPPH) and Trolox (Merck KgaA, Darmstadt, Germany) were used.
In order to quantify the amount of phenolic compounds present in the extract, gallic acid, Folin–Ciocalteu reagent and sodium carbonate (Merck KgaA, Darmstadt, Germany) were employed.
Two solvents were employed to separate the constituents of the extracts as follows: HPLC-grade acetonitrile (Panreac S.L.U, Castellar del Vallés, Spain) and Milli-Q water, both acidified using 2% glacial acetic acid (Panreac S.L.U, Castellar del Vallés, Spain). Quercetin 3-O-glucoside (Q3GLU) (Merck KgaA, Darmstadt, Germany), were used as standard for the quantification.
2.3. Enzymatic Extraction
2.3.1. Extraction Equipment
The equipment used for the extraction was a Nahita LNB001 (Auxilab S.L., Navarra, Spain) incubator fitted with a touch screen that allows digitally setting up agitation, temperature and time values.
2.3.2. Extraction Procedure
Several factors were considered for the optimization of the extraction method as follows: solvent composition (0−40% ethanol in water) and pH (4.0−6.0), agitation (50−200 rpm), temperature (40−60 °C), sample-to-solvent ratio (0.1−0.2 g in 15 mL solvent), enzyme-to-sample ratio (100−1000 U/g) and extraction time (10−60 min). Levels for each factor were stablished according to previous studies of our research group [
36]. The enzyme amount was determined according to other studies of enzymatic extraction with pectinases [
21].
The samples for the extractions were weighted and mixed with the corresponding solvent for each experiment. Then, the enzyme was added, and the extraction conditions were set up to proceed with the extraction. Once the extraction had been completed, the resulting extracts were centrifuged twice (1702× g, 5 min). The supernatant was collected, made up to 25 mL and kept in Falcon tubes until further analysis.
2.4. Phenolic Compounds Quantification
The compounds were separated by means of an ACQUITY UPLC® H-Class System (Waters Corporation, Milford, MA, USA). This equipment consists of a quaternary elution system (Quaternary Solvent Manager) coupled to a photodiode array detector (PAD eλ Detector, Waters Corporation, Milford, MA, USA). The column used for the separation was an ACQUITY UPLC® BEH C18 (1.7 μm, 2.1 mm × 100 mm, Waters, Milford, MA, USA). The equipment was controlled through the software application EmpowerTM 3 (Waters Corporation, Milford, MA, USA).
In order to determine and quantify the phenolic compounds in the extract, 3.0 μL samples were injected into the column, and the eluent was allowed to flow at 0.6 mL min
−1. The eluent consisted of a mixture of Milli-Q water and HPLC-grade acetonitrile, both acidified using 2% glacial acetic acid. The gradient used has already been described by Yerena-Prieto et al. [
36]: 0 min, 0% B; 1 min, 5% B; 2 min, 10% B; 3 min, 15% B; 4 min, 20% B; 5 min, 30% B; 7 min, 35% B; 8 min, 40% B; 10 min, 75% B and 12 min, 0% B. The total analysis time, including the return to the initial conditions and re-equilibration, spanned 15.0 min.
The compounds were quantified at
λ = 350 nm, based on a calibration curve (
y = 6007.6
x + 1930.3;
R2 = 0.9992) generated by 0.5, 1, 5, 10 and 50 mg L
−1 Q3GLU in methanol, as this is one of the main phenolic compounds produced by
M. oleifera [
30]. The results were therefore expressed as milligrams of Q3GLU equivalents per gram of dried leaves (mg Q3GLUE/g).
2.5. Extraction Method
2.5.1. Placket–Burman Experimental Design
The Placket–Burman Experimental Design is a screening method that allows researchers to reduce the number of factors required for an experimental design by pointing out which of the factors has a significant influence. Thus, based on a statistical algorithm, the number of experiments required to identify which relevant factors can be reduced [
37]. In this particular case, instead of the 128 (2
7) experiments that would be required for a factorial design determined by 7 factors and 2 levels (−1.0, lower and 1.0 higher), just 12 experiments were needed to determine the factors to be taken into account for an optimal procedure (
Table 1).
As already mentioned in
Section 2.3.2, the factors selected for this study were time (
X1, expressed as min), pH (
X2), temperature (
X3, expressed as °C), agitation (
X4, expressed as revolutions per minute) solvent composition (
X5, expressed as ethanol percentage), sample-to-solvent ratio (
X6, expressed as grams sample per 15 mL solvent) and enzyme-to-sample ratio (
X7, expressed as units of enzyme per gram sample). The response variable (
Y) for the design of the method was the sum of the peak areas, given that the ultra-high-performance liquid chromatography-photodiode array detector (UHPLC-PDA) method is more reliable than other colorimetric quantification techniques.
2.5.2. Box–Behnken Experimental Design
Once the most significant factors had been identified, it was necessary to determine the optimal value for each factor. A Box–Behnken Design determined by 4 factors (solvent pH (
X2), temperature (
X3), solvent composition (
X5) and enzyme-to-sample ratio (
X7)) at 3 levels (−1.0, low; 0, medium and 1.0, high) (
Table 2) was employed for that purpose. As already mentioned in
Section 2.5.1., the sum of the peak areas related to the mass of dry sample employed was considered as the response variable (
Y) to be optimized for the design of the extraction method.
This statistical design allows reducing the number of experiments to 27 compared to the 81 (3
4) experiments that would have been required for an equivalent factorial design. Thus, the maximum information is obtained from a relatively shorter number of experiments. This is a spherical design, where the distance from the experimental points to the central one is α = √2, while no experiments under extreme conditions are required, which is rather convenient, since those conditions that might threaten the integrity of some of the compounds in the samples, such as high temperatures, are left out [
37].
The experimental results were adjusted to a surface-response polynomium (Equation (1)) where 𝛽𝑖 is the coefficient assigned to the main effects; 𝛽𝑖𝑗, to the interaction effects; 𝛽𝑖𝑖, to the quadratic factors, Xi and Xj correspond to each factor, and r is the residual value. The fit of the model is indicated by the R2 coefficient obtained, and the statistical significance of each factor can be determined through an analysis of variance (ANOVA). The data obtained from all the experiments were analyzed by means of the statistical software application STATGRAPHICS XVI (Statgraphics Technologies, Inc., The Plains, VA, USA).
2.5.3. Determining the Extraction Time
After establishing the optimal extraction conditions, a single-factor study was performed in order to determine the optimal extraction time. For that purpose, a number of extractions under the established optimal conditions were performed in triplicate using 2, 5, 10, 15, 20 and 25 min.
2.5.4. Repeatability and Intermediate Precision
Three extraction batches of 8 replicates each were performed under the established optimal conditions in order to evaluate the repeatability and the intermediate precision of the developed method. Each batch was subjected to extraction on a different day so that the relative standard deviation (RSD) corresponding to the intragroup repeatability (within each batch) and the RSD corresponding to the intergroup intermediate precision could be determined.
2.6. Determining the Antioxidant Compounds Content
The flavonoids content in the final extracts that had been obtained under the established optimal conditions was measured in order to assess the antioxidant properties of the extracts and the suitability of the extraction method for the intended purpose.
2.6.1. Quantifying the Antioxidant Compounds through Ultra-High Performance Liquid Chromatography (UHPLC)
The flavonoids were identified through their chromatograms at 350 nm (
Figure 1). Only the compounds that could be detected at a retention time between 3.60 and 4.50 min were considered, as this is the region where these compounds are to be found when this chromatographic method is used [
30].
This chromatographic method was used to identify the compounds based on their retention times and according to previous studies completed by our research group [
30], and the results were expressed as milligrams of Q3GLU per gram sample, as this is the main phenolic compound produced by moringa.
2.6.2. Evaluation of the Antioxidant Potential of the Extracts through Colorimetric Methods
In addition to the UHPLC-PDA quantification, the antioxidant activity of the final extracts was determined using two different colorimetric methods: free radical scavenging activity through a 2,2-diphenyl-1-pycrylhydrazile (DPPH) assay and total phenolic content through a Folin–Ciocalteu assay.
Determining the Free Radical Scavenging Activity
This assay was performed as follows: a 100 μL sample was gently mixed with 2 mL of a 6 × 10
−5 M stock solution of DPPH. The reaction was left in the absence of light for 40 min, and then its absorbance at
λ = 515 nm was measured by means of a UV-Vis Helios-γ-Unicam spectrophotometer (Thermo Scientific, Waltham, MA, USA) in 10 mm-width cuvettes. A blank solution was prepared by replacing the sample with distilled water. The free radical scavenging activity was determined according to Equation (2), where
C is the free radical scavenging activity;
A0, the blank absorbance and
AS the absorbance of the sample, both absorbances measured at 515 nm.
Once the free radical scavenging activity had been determined, the concentration of the antioxidant compounds could be measured based on a calibration curve (
y = 88.941
x + 0.7478;
R2 = 0.9959) obtained by measuring the free radical scavenging activity of the Trolox standard solutions at 0.0, 0.3, 0.6, 0.9 and 1.1 mM. Trolox is widely used as a standard for antioxidant-determining assays [
38,
39,
40,
41], as it is the hydrosoluble analogue of vitamin E [
42]. Consequently, the results were expressed in terms of milligrams of Trolox equivalents per gram sample (mg TE/g).
Determining Total Phenolic Content (TPC)
The TPC can be determined by attending to the interpolation of the absorbance data of the calibration curve (
y = 0.0015
x + 0.0059;
R2 = 0.9999) previously generated and by measuring the TPC of a number of gallic acid solutions at 25, 50, 100, 250, 500 and 1000 mg L
−1, since gallic acid is a phenolic compound typically employed as the reference for these assays [
43,
44,
45]. The results are then expressed as milligrams of gallic acid equivalents per gram sample (mg GAE/g).