# Extraction and Physicochemical Characterization of Mucilage fromOpuntia cochenillifera (L.) Miller

Authors: Mariel Monrroy; Erick García; Katherine Ríos; José Renán García
Journal: Journal of Chemistry
 (2017)

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## Abstract

The aim of this study was to extract mucilage fromO. cochenillifera (L.) cacti and determine its functional and physicochemical properties. The best mucilage yield (31%) was obtained by nonthermal extraction with hydration. The mucilage has appreciable carbohydrate and protein contents. The phytochemical analysis shown the presence of alkaloids and terpenes/steroids. The Fourier transformed infrared (FT-IR) spectrum of the mucilage exhibits typical bands for carbohydrates as O–H, C–H, and –COO−. The mucilage demonstrated water- and oil-holding capacities of 2.78 g water/g dry mucilage and 1.80 g oil/g dry mucilage, respectively, these properties can have a positive effect on the texture of the products when used as a stabilizer. The mildly acidic pH (4.8–5) contributes to its emulsifying capacity. The presence of electrolytes in the mucilage can be of great value in flocculation processes. The mucilage forms low viscosity solutions in the same manner as gum Arabic. Finally, its potential for use as a textile dye remover was evaluated, achieving a 70% removal rate from aqueous solutions. The prepared mucilage exhibits properties that recommend it as a natural material that can be used as an additive in the chemical, food, pharmaceuticals and cosmetics industries, as well as in decontamination processes.


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## Body

## 1. Introduction

Opuntia spp. are flowering plants belonging to the Cactaceae family. They grow naturally in tropical and semitropical regions [1], and their cultivation is well known, especially in Mexico, Argentina, Peru, Bolivia, Brazil, Chile, the United States (Texas), Spain, Italy, Africa (Morocco, Tunisia, Eritrea, and Ethiopia), Israel, and South Africa [2]. Traditionally, theOpuntia have been used for both medicinal and edible purposes. Research has shown that extracts from their pads can reduce cholesterol levels [3] and exhibit hypoglycemic effects [4], antiulcer activity [5], neuroprotective effects [6], and anti-inflammatory and analgesic properties [5, 7]. Furthermore, these Cactaceae are characterized by their hydrocolloid properties, having a high capacity to retain water under adverse weather conditions due largely to one of their main functional components, mucilage [1, 2].Mucilage is a complex polymeric substance composed mainly of carbohydrates with highly branched structures, which includel-arabinose,d-galactose,l-rhamnose,d-xylose, and galacturonic acid in various proportions [8]. It also contains glycoproteins [9] and other substances such as tannins, alkaloids, and steroids [1]. The mucilage composition differs among the variousOpuntia spp. and the regions in which they grow [1, 2]. In addition to the aforementioned medicinal activities for these cacti, which are associated with this complex material, the ability of mucilage to form molecular networks and retain large amounts of water makes it a potential source of hydrocolloids for the chemical and cosmetics industries. Several studies have evaluated its uses in water purification/filtration [2, 9], as an adhesive lime [Ca(OH)2] [3], emulsifying agent [10], or flocculant [11], and as an enhancer of water infiltration in soils, due to its physical properties (viscosity, elasticity, texture, and emulsifier) [12]. Other mucilage applications include its use in foods as a stabilizer, flavoring agent, fat substitute [2], and edible coating to extend the useful life of fruit [13].Most studies on the physical and chemical properties ofOpuntia mucilage have focused onO. ficus-indica, and there is little scientific information on the characteristics of otherOpuntia spp. such asO. cochenillifera. Among the meritorious attributes ofO. cochenillifera are its hypoglycemic effects [4] and the ability to decolorize water [14]. Consequently, this research will focus on optimizing the extraction of the mucilage fromO. cochenillifera (L.) Miller and its physicochemical characterization. The mucilage thus obtained could be a natural, economical alternative functional material for use in many industrial processes.


## 2. Experimental

### 2.1. Raw Material

Fresh cladodes ofO. cochenillifera were harvested from Universidad Autónoma de Chiriquí-Panamá (8°25′49.51′′N y 82°26′53.36′′W). The cladodes had an average size of 7.67 cm × 18.15 cm. Moisture content was determined after drying at 105°C for 24 h. The specimen was identified by Professor Rafael Rincón at the Herbarium of Universidad Autónoma de Chiriquí (code: UCH). A voucher specimen (number: 006757) was deposited in the Herbarium.


### 2.2. Extraction of Mucilage

#### 2.2.1. Thermal Extraction of Fresh Cladodes

The cladodes were peeled, cut into pieces (2 × 2 cm2), crushed, and homogenized in a ratio of 7.5 g in 15 ml distilled water. This ratio was equivalent to suspending 100 mg dry basis in 5 ml water. Samples were placed in a water bath at different temperatures for various reaction times (Table 1) and then filtered. The mucilage was precipitated by adding 45 mL ethanol and dried in an oven at 60°C.Table 1
Thermal extraction conditions for fresh and dried cladodesofO. cochenillifera.
Experiment number
Time(min)
Temperature(°C)
1
60
50
2
90
50
3
60
80
4
90
80
5
54
65
6
96
65
7
75
44
8
75
86
9
75
65
10
75
65
11
75
65


#### 2.2.2. Thermal Extraction of Dried Cladodes

The cladodes were cut into pieces (2 × 2 cm2), dried at 60°C for 48 h, and milled. Then, the mucilage was extracted by mixing 100 mg of the milled sample with 5 mL water for different temperatures (44–86°C, T) and times (54–96 min, t) (Table 1). The mucilage was precipitated by adding 15 mL ethanol and dried in an oven at 60°C.The influence of the variablesT and t for both types of extraction was determined using response surface methodology (RSM) and multiple linear regression methods. The optimum conditions for extracting the mucilage were obtained as the maximum values of the response surface by the SIMPLEX method. The generation and evaluation of the experimental designs were carried out with the program Modde 7.0.0.1 (Umetrics, USA). Statistical validation was performed using one-way analysis of variance ANOVA with a confidence level of 95%. The models obtained were based on a circumscribed central composite design made of a factorial design and star points.


#### 2.2.3. Extraction by Hydration

A solution was prepared by mixing the milled sample (100 mg) with water (5 mL) and allowing it to stand for 24 h. Then, the solution was filtered and the mucilage was precipitated by adding 15 mL ethanol and dried in an oven at 60°C.


#### 2.2.4. Extraction by Agitation

A solution was prepared as described in the preceding section, stirred for 30 min using a magnetic stirrer, and then filtered. The mucilage was precipitated by adding 15 mL ethanol for 30 min and dried in an oven at 60°C.


#### 2.2.5. Extraction by Agitation and Hydration

In this extraction, the sample was hydrated and agitated as in the previous sections.All extractions were performed in triplicate. The results were analyzed using ANOVA and Tukey’s honest significant difference (HSD) multiple comparison test (p≤0.05).


### 2.3. Chemical Characterization of the Mucilage

The total carbohydrate content was determined by the phenol-sulfuric acid method, and the visible absorption of the resulting solution was measured at 490 nm (modified method of Bartkiene [15]). For the quantitative carbohydrate determination, mucilage powder (100 mg) and 2.5 N HCl (5 mL) were mixed in a test tube and placed in a water bath at 95°C for 3 h. The solution was neutralized with sodium carbonate, diluted with water (5 mL), and centrifuged. The supernatant was brought to a volume of 100 mL. Then, a portion of the sample (0.1 mL) was added to 5% phenol (1 mL) and concentrated sulfuric acid (5 mL), vortexed for 1 min, and placed in a water bath at 30°C for 20 min. Finally, the total carbohydrate content was determined by visible spectrophotometry (Vis) at a wavelength of 490 nm and quantified against a calibration curve using glucose. The total nitrogen concentration in the mucilage was determined by the Kjeldahl method. The mineral contents were quantified by atomic absorption spectroscopy. All analyses were performed in triplicate.The mucilage was subjected to a phytochemical screening using the following tests: the Salkowski test for sterols; the Shinoda and sodium hydroxide tests for flavonoids; the Dragendorff, Wagner, and Mayer tests for alkaloids; the ferric chloride test for tannins; the Rosenthaler test for saponins; and the Dimroth test for 5-hydroxy flavones. A thin-layer chromatography (TLC) was used in the analysis of alkaloids. TLC was performed on 10 × 3 cm silica gel plates with a fluorescent indicator at 254 nm (Applichem, USA). Chloroform/methanol (9 : 1), chloroform (100%), and ethyl acetate/methanol/chloroform/hexane (6 : 1 : 2 : 1) were used as mobile phases. Mucilage sample was dissolved in methanol/chloroform (1 : 1), macerated for 24 hours, and then centrifuged. Solution (25μL) was carefully layered at 1 cm from the bottom of the plate. After the separation, plates were dried at 60°C for 5 min. Then drying, the spots on the developed plates were visualized at 254 nm and also revealed with Dragendorff and Wagner reagents. A meter rule was used to measure the distance moved by the solvent and distance moved by spot, from which the retention factor (Rf values) of the spots was calculated.Infrared spectra of the mucilage were measured by direct transmittance using the KBr pellet technique. Spectra were recorded between 4000 and 500 cm−1, using a Shimadzu IRAffinity-1 Fourier-transform infrared spectrometer (FT-IR) equipped with a deuterated L-alanine doped triglycine sulfate (DLATGS) detector. The background used for the FT-IR measurements was a KBr pellet that contained no sample. All spectra were measured at a spectral resolution of 2 nm and 32 scans were taken per sample.


### 2.4. Physical Characterization of the Mucilage

The conductivity, pH, density, and viscosity were determined in mucilage solutions of 1, 4, and 6% (w/v), prepared by dissolving the mucilage powder in distilled water. Conductivity was determined using a conductometer and the pH with a pH meter (Mettler–Toledo, USA). The density was determined using a glass pycnometer. The viscosity of the samples, measured with a calibrated Cannon-Fenske glass capillary viscometer (Cannon Instrument Co., State College, PA, USA), was determined as the time required for the sample to flow under gravity through the device. All tests were performed in triplicate.The water-holding capacity (WHC) and oil-holding capacity (OHC) were determined according to the methods of Chau et al. [16] and Thanatcha and Pranee [17]. A mucilage powder sample (0.2 g) was mixed in 10 mL distilled water or olive oil by vortexing for 1 min and centrifuged at 2200 rpm for 30 min. Then, the supernatant was removed and weighed. The WHC was expressed as the grams water held per gram sample, and the OHC as the grams oil held per gram sample.


### 2.5. Decolorization of a Textile Dye Solution

Different amounts of mucilage (0.1, 0.2, or 0.3 g) were mixed with separate green and blue dye solutions (10 mL, 100 ppm, Dylon Fabric Dye) by vortexing for 3 min and then centrifuged at 3000 rpm for 5 min. The supernatants were removed and subjected to absorbance measurements by Vis spectrophotometry at 586 nm (green) and 400 nm (blue). The percentage removal of the dye solution was then determined.


## 2.1. Raw Material

Fresh cladodes ofO. cochenillifera were harvested from Universidad Autónoma de Chiriquí-Panamá (8°25′49.51′′N y 82°26′53.36′′W). The cladodes had an average size of 7.67 cm × 18.15 cm. Moisture content was determined after drying at 105°C for 24 h. The specimen was identified by Professor Rafael Rincón at the Herbarium of Universidad Autónoma de Chiriquí (code: UCH). A voucher specimen (number: 006757) was deposited in the Herbarium.


## 2.2. Extraction of Mucilage

### 2.2.1. Thermal Extraction of Fresh Cladodes

The cladodes were peeled, cut into pieces (2 × 2 cm2), crushed, and homogenized in a ratio of 7.5 g in 15 ml distilled water. This ratio was equivalent to suspending 100 mg dry basis in 5 ml water. Samples were placed in a water bath at different temperatures for various reaction times (Table 1) and then filtered. The mucilage was precipitated by adding 45 mL ethanol and dried in an oven at 60°C.Table 1
Thermal extraction conditions for fresh and dried cladodesofO. cochenillifera.
Experiment number
Time(min)
Temperature(°C)
1
60
50
2
90
50
3
60
80
4
90
80
5
54
65
6
96
65
7
75
44
8
75
86
9
75
65
10
75
65
11
75
65


### 2.2.2. Thermal Extraction of Dried Cladodes

The cladodes were cut into pieces (2 × 2 cm2), dried at 60°C for 48 h, and milled. Then, the mucilage was extracted by mixing 100 mg of the milled sample with 5 mL water for different temperatures (44–86°C, T) and times (54–96 min, t) (Table 1). The mucilage was precipitated by adding 15 mL ethanol and dried in an oven at 60°C.The influence of the variablesT and t for both types of extraction was determined using response surface methodology (RSM) and multiple linear regression methods. The optimum conditions for extracting the mucilage were obtained as the maximum values of the response surface by the SIMPLEX method. The generation and evaluation of the experimental designs were carried out with the program Modde 7.0.0.1 (Umetrics, USA). Statistical validation was performed using one-way analysis of variance ANOVA with a confidence level of 95%. The models obtained were based on a circumscribed central composite design made of a factorial design and star points.


### 2.2.3. Extraction by Hydration

A solution was prepared by mixing the milled sample (100 mg) with water (5 mL) and allowing it to stand for 24 h. Then, the solution was filtered and the mucilage was precipitated by adding 15 mL ethanol and dried in an oven at 60°C.


### 2.2.4. Extraction by Agitation

A solution was prepared as described in the preceding section, stirred for 30 min using a magnetic stirrer, and then filtered. The mucilage was precipitated by adding 15 mL ethanol for 30 min and dried in an oven at 60°C.


### 2.2.5. Extraction by Agitation and Hydration

In this extraction, the sample was hydrated and agitated as in the previous sections.All extractions were performed in triplicate. The results were analyzed using ANOVA and Tukey’s honest significant difference (HSD) multiple comparison test (p≤0.05).


## 2.2.1. Thermal Extraction of Fresh Cladodes

The cladodes were peeled, cut into pieces (2 × 2 cm2), crushed, and homogenized in a ratio of 7.5 g in 15 ml distilled water. This ratio was equivalent to suspending 100 mg dry basis in 5 ml water. Samples were placed in a water bath at different temperatures for various reaction times (Table 1) and then filtered. The mucilage was precipitated by adding 45 mL ethanol and dried in an oven at 60°C.Table 1
Thermal extraction conditions for fresh and dried cladodesofO. cochenillifera.
Experiment number
Time(min)
Temperature(°C)
1
60
50
2
90
50
3
60
80
4
90
80
5
54
65
6
96
65
7
75
44
8
75
86
9
75
65
10
75
65
11
75
65


## 2.2.2. Thermal Extraction of Dried Cladodes

The cladodes were cut into pieces (2 × 2 cm2), dried at 60°C for 48 h, and milled. Then, the mucilage was extracted by mixing 100 mg of the milled sample with 5 mL water for different temperatures (44–86°C, T) and times (54–96 min, t) (Table 1). The mucilage was precipitated by adding 15 mL ethanol and dried in an oven at 60°C.The influence of the variablesT and t for both types of extraction was determined using response surface methodology (RSM) and multiple linear regression methods. The optimum conditions for extracting the mucilage were obtained as the maximum values of the response surface by the SIMPLEX method. The generation and evaluation of the experimental designs were carried out with the program Modde 7.0.0.1 (Umetrics, USA). Statistical validation was performed using one-way analysis of variance ANOVA with a confidence level of 95%. The models obtained were based on a circumscribed central composite design made of a factorial design and star points.


## 2.2.3. Extraction by Hydration

A solution was prepared by mixing the milled sample (100 mg) with water (5 mL) and allowing it to stand for 24 h. Then, the solution was filtered and the mucilage was precipitated by adding 15 mL ethanol and dried in an oven at 60°C.


## 2.2.4. Extraction by Agitation

A solution was prepared as described in the preceding section, stirred for 30 min using a magnetic stirrer, and then filtered. The mucilage was precipitated by adding 15 mL ethanol for 30 min and dried in an oven at 60°C.


## 2.2.5. Extraction by Agitation and Hydration

In this extraction, the sample was hydrated and agitated as in the previous sections.All extractions were performed in triplicate. The results were analyzed using ANOVA and Tukey’s honest significant difference (HSD) multiple comparison test (p≤0.05).


## 2.3. Chemical Characterization of the Mucilage

The total carbohydrate content was determined by the phenol-sulfuric acid method, and the visible absorption of the resulting solution was measured at 490 nm (modified method of Bartkiene [15]). For the quantitative carbohydrate determination, mucilage powder (100 mg) and 2.5 N HCl (5 mL) were mixed in a test tube and placed in a water bath at 95°C for 3 h. The solution was neutralized with sodium carbonate, diluted with water (5 mL), and centrifuged. The supernatant was brought to a volume of 100 mL. Then, a portion of the sample (0.1 mL) was added to 5% phenol (1 mL) and concentrated sulfuric acid (5 mL), vortexed for 1 min, and placed in a water bath at 30°C for 20 min. Finally, the total carbohydrate content was determined by visible spectrophotometry (Vis) at a wavelength of 490 nm and quantified against a calibration curve using glucose. The total nitrogen concentration in the mucilage was determined by the Kjeldahl method. The mineral contents were quantified by atomic absorption spectroscopy. All analyses were performed in triplicate.The mucilage was subjected to a phytochemical screening using the following tests: the Salkowski test for sterols; the Shinoda and sodium hydroxide tests for flavonoids; the Dragendorff, Wagner, and Mayer tests for alkaloids; the ferric chloride test for tannins; the Rosenthaler test for saponins; and the Dimroth test for 5-hydroxy flavones. A thin-layer chromatography (TLC) was used in the analysis of alkaloids. TLC was performed on 10 × 3 cm silica gel plates with a fluorescent indicator at 254 nm (Applichem, USA). Chloroform/methanol (9 : 1), chloroform (100%), and ethyl acetate/methanol/chloroform/hexane (6 : 1 : 2 : 1) were used as mobile phases. Mucilage sample was dissolved in methanol/chloroform (1 : 1), macerated for 24 hours, and then centrifuged. Solution (25μL) was carefully layered at 1 cm from the bottom of the plate. After the separation, plates were dried at 60°C for 5 min. Then drying, the spots on the developed plates were visualized at 254 nm and also revealed with Dragendorff and Wagner reagents. A meter rule was used to measure the distance moved by the solvent and distance moved by spot, from which the retention factor (Rf values) of the spots was calculated.Infrared spectra of the mucilage were measured by direct transmittance using the KBr pellet technique. Spectra were recorded between 4000 and 500 cm−1, using a Shimadzu IRAffinity-1 Fourier-transform infrared spectrometer (FT-IR) equipped with a deuterated L-alanine doped triglycine sulfate (DLATGS) detector. The background used for the FT-IR measurements was a KBr pellet that contained no sample. All spectra were measured at a spectral resolution of 2 nm and 32 scans were taken per sample.


## 2.4. Physical Characterization of the Mucilage

The conductivity, pH, density, and viscosity were determined in mucilage solutions of 1, 4, and 6% (w/v), prepared by dissolving the mucilage powder in distilled water. Conductivity was determined using a conductometer and the pH with a pH meter (Mettler–Toledo, USA). The density was determined using a glass pycnometer. The viscosity of the samples, measured with a calibrated Cannon-Fenske glass capillary viscometer (Cannon Instrument Co., State College, PA, USA), was determined as the time required for the sample to flow under gravity through the device. All tests were performed in triplicate.The water-holding capacity (WHC) and oil-holding capacity (OHC) were determined according to the methods of Chau et al. [16] and Thanatcha and Pranee [17]. A mucilage powder sample (0.2 g) was mixed in 10 mL distilled water or olive oil by vortexing for 1 min and centrifuged at 2200 rpm for 30 min. Then, the supernatant was removed and weighed. The WHC was expressed as the grams water held per gram sample, and the OHC as the grams oil held per gram sample.


## 2.5. Decolorization of a Textile Dye Solution

Different amounts of mucilage (0.1, 0.2, or 0.3 g) were mixed with separate green and blue dye solutions (10 mL, 100 ppm, Dylon Fabric Dye) by vortexing for 3 min and then centrifuged at 3000 rpm for 5 min. The supernatants were removed and subjected to absorbance measurements by Vis spectrophotometry at 586 nm (green) and 400 nm (blue). The percentage removal of the dye solution was then determined.


## 3. Results and Discussion

The mucilage content in a cladode is directly related to the moisture content because its heteropolysaccharide components have the ability to absorb water. In this work, the moisture content in young cladodes was higher than in older cladodes; thus, young cladodes with an average size of 7.67 cm × 18.15 cm were employed. The moisture content in the fresh cladodes ofO. cochenillifera is 92%.As mentioned earlier, mucilage could be a natural, economical alternative material for many industrial processes; therefore, an investigation of extraction process efficiency is relevant. Different extraction processes were examined, such as thermal and nonthermal extraction (hydration and agitation).


### 3.1. Mucilage Extraction

The mucilage yields obtained from fresh and dried cladodes using thermal extraction varied from 22 to 25% and 20 to 33% on a dry matter basis (Table2), respectively. From the experimental design data and mucilage percentage obtained under each condition (Table 4), quadratic polynomials were determined (see (1)) for the fresh and dried cladodes, respectively, and validated by the ANOVA test.(1)Mucilagefresh,%=22.0±0.3+0.3±0.2t+0.02±0.2T+0.7±0.2t2-0.7±0.3tT,Mucilagedried,%=21.3±1.5-2.1±1.3T+4.6±1.4T2,where t is time and T temperature.Table 2
Mucilage yields fromO. cochenillifera obtained via thermal extraction.
Experiment number
Yield
Yield
(%)a
(%)b
1
21.7
27.4
2
23.8
29.0
3
23.3
24.0
4
22.1
13.2
5
23.6
21.1
6
24.6
19.6
7
22.1
33.0
8
22.3
27.2
9
21.9
24.1
10
21.8
20.5
11
22.4
21.1
aFresh cladodes.
bDried cladodes.In the case of the fresh cladodes, the linear term for time has a positive coefficient, meaning that the mucilage extraction increases with time. The positive quadratic terms indicates that large variation of time in either direction will result in extraction yield increase (the response surface shows a minimum). However, the linear term for temperature has no effect on mucilage yield, but considering the confidence intervals, the interaction between both variables has a significant effect on mucilage extraction. For the dried cladodes, the linear term for the temperature has a negative coefficient, meaning that the extraction yield increased as the temperature declined. The positive quadratic terms indicates that large variation of temperature in either direction will result in extraction yield increase. Time appears to have no significant effect on mucilage extraction for the range studied (50–80 min). Considering the confidence intervals, the interactions between variables have no significant effect on mucilage extraction.Error values corresponded to a 95% confidence level. The effects of the extraction conditions on the mucilage yield are shown in the response surface graph for the polynomials (within the studied variable ranges) (Figures1(a) and 1(b)). The responses are close to the experimental values, with correlation coefficients (r2) of 0.93 and 0.89 for the fresh and dry cladodes, respectively.Figure 1
Response surfaces for removal of mucilage extracted fromO. cochenillifera: (a) fresh cladodes and (b) dry cladodes.
(a)
(b)The optimum values of the variables for the maximal mucilage yields were determined by the SIMPLEX method using the maximum values of the response surface. The maximum mucilage yields predicted for the fresh and dried cladodes are24.5±0.3% and 34±1%. The predicted values of the best extraction variables are 54 min and 80°C for the fresh cladodes and 86 min and 44°C for the dried cladodes. The experimental mucilage yields for the fresh and dried cladodes obtained under these conditions are 24±1% and 31±2%, respectively, which agree well with the predicted values. Mucilage extraction from the dried cladodes was better than from the fresh cladodes, which may be related to the larger surface area of the former, which would improve the extraction process.The nonthermal methods of extraction from the cladodes were based on hydration, agitation, and hydration and agitation processes. Table3 shows the mucilage yields obtained for the three approaches. Increased performance is observed for the samples subjected to the hydration and hydration/agitation processes, compared to agitation alone. This indicates that the hydration process is very important when mucilage extraction is performed with previously dried and powdered cladode samples. The results obtained were analyzed using ANOVA and Tukey’s HSD multiple comparison test (p≤0.05), which showed that there is a significant difference between the mean of the agitation process with the other two processes at the 95% confidence level.Table 3
Mucilage yields via nonthermal extraction fromO. cochenillifera cladodes.
Treatment
Yield (%)
Hydration
31 ± 1
Agitation
26.4 ± 0.1
Hydration and agitation
31 ± 2Table 4
Mineral content of mucilagefromO. cochenillifera.
N
P
K
Ca
Mg
%
1.6
0.4
1.2
1.8
0.3
Fe
Cu
Mn
Zn
Na
Mg·kg−1
191
424
344
386
250The maximum mucilage extraction yields obtained from cladodes under the thermal and nonthermal extraction methods in this study are similar and/or higher than those reported for otherOpuntia such asO. streptacantha (7.2%),O. megacantha (7.4%),O. albicarpa (6.9%),O. milpa alta (7%),O. dillenii(16%), andO. ficus-indica (4–25%) [8, 18–20].


### 3.2. Chemical Characterization of the Mucilage

The total carbohydrate content was 40%, which is higher than that reported forO. dillenii, with 12 to 15% as polysaccharides [20], but within the range given forO. ficus-indica (13–64%) [21, 22]. In addition, the mucilage is an excellent source of essential minerals such as calcium, phosphorus, magnesium, iron, potassium, zinc, and copper (Table 4). Calcium is the most abundant mineral in the mucilage, which agrees with other studies of cactus pads [23–25]. For example,O. ficus-indica was a better source of calcium than spinach, soy, and grains, suggesting thatOpuntia spp. may have potential in the prevention and treatment of diseases such as osteoporosis [26]. Because of their excellent nutritional qualities,Opuntia (especiallyO. indica) have been used as food sources in countries such as Mexico. As theO. cochenillifera mucilage is a rich source of carbohydrates and essential minerals, it has good potential for use as a nutritional supplement.The crude protein content was determined as 7.4%. This value is comparable to those reported forO. ficus-indica cladodes (5–9%) but higher than those inO. stricta (5%) and guar gum (3–5%) [1, 27, 28]. The interactions that occur through the specific (hydrophilic) functional groups of polysaccharides and proteins are an important factor in the study of mucilage proteins; these form a three-dimensional network that can improve the stability and uniformity of the system matrix and suggest potential application in the industry [29]. Usually, proteins and polysaccharides are safe food additives that can form physically stable emulsions [30].The phytochemical analysis shown in Table5 reveals the presence of alkaloids by the Dragendorff, Mayer, and Wagner tests, which identify quaternary alkaloids and/or amine-oxides. The TLC analysis also revealed the presence of alkaloids; two spots were visualized at 254 nm (Figure 2), using different mixtures of eluents. Ethyl acetate/methanol/chloroform/hexane (6 : 1 : 2 : 1) is the best eluent employed, showing Rf values 0.88 and 0.63, respectively (Table 6). Likewise, two spots were observed with Dragendorff and Wagner reagents. The presence of terpenes/steroids was also found using the Salkowski test. Although the presence of saponins, flavonoids, and tannins was not found in this study, Tomás Ch et al. [31] reported the presence of saponins, flavonoids, and alkaloids in the pulp ofO. ficus-indica. The chemical composition of theOpuntiaspp. is quite variable, depending on a number of factors such as the chemical characteristics of the soil, geographical location, environmental conditions, age, and species [8, 22, 27].Table 5
Phytochemical analysis ofO. cochenillifera mucilage.
Metabolite
Test
Mucilage
Alkaloids
Meyer
(+)
Dragendorff
(+)
Wagner
(+)
Saponins
Rosenthaler
(−)
Tannins
FeCl3
(−)
Terpenes/steroids
Salkowski
(+)
Flavonoids
Reaction with NaOH
(−)
Shinoda
(−)
5-hydroxy flavones
Dimroth
(−)Table 6
Alkaloids analysis ofO. cochenillifera mucilage by TLC.
Eluent
Number of spots detected
Rf 1
Rf 2
Observation
Chloroform/methanol (9 : 1)
2
0.70
0.93
Brown spots with Dragendorff and Wagner reagent; fluoresced violet light at 254 nm.
Chloroform (100%)
2
0.70
0.82
Ethyl acetate/methanol/chloroform/hexane (6 : 1 : 2 : 1)
2
0.63
0.88Figure 2
TLC based detection of alkaloids ofO. cochenillifera mucilage extracts visualized under UV at 254 nm.The FT-IR spectrum of the mucilage exhibits typical bands forOpuntiaspp. The functional group bands found in theO. cochenilliferamucilage (Figure 3) are characteristic for proteins and polysaccharides. The bands at 3420, 2931, and 1623 cm−1 represent the stretching vibrations of O–H, C–H, and –COO− (asymmetric vibrations) groups, respectively, in carbohydrate and uronic acid molecules. Further, the bands at 2931 and 1623 cm−1 appear to be associated with the N–H stretching and bending motions, respectively, of proteins. Han et al. [20] and Contreras-Padilla et al. [18] reported bands at 3500–3200 cm−1 corresponding to carbohydrate O–H bonds inO. dillenii andO. ficus-indicamucilage. Also, they assigned a band around 2920 cm−1 to the C–H stretching vibration of the pyranose group. Zhao et al. [32] attributed the bands at 1620, 1596, and 1420 cm−1 to deprotonated carboxylic acid groups (–COO−) in uronic acid inO. monacantha.Similar bands are observed at 1623, 1582, and 1431 cm−1 in our spectrum. The bands found at ~1431–1264 cm−1 can be assigned to C–O stretching and O–H deformation vibrations, according to Han et al. [20] and the bands at 1431–1393 cm−1 indicate C–N stretching modes [33]. The bands at 1085 and 1045 cm−1 indicate the presence of monosaccharides such as mannose and glucose in pyranose ring conformations [20, 34]. The absorption band at 893 cm−1 corresponds to β-d-glucose [32]. The bands at 774 and 608 cm−1 are attributed to N–H and O–H out-of-plane vibrations, respectively [32, 33].Figure 3
FT-IR spectrum ofO. cochenillifera mucilage.


### 3.3. Physical Characterization of the Mucilage

#### 3.3.1. pH, Conductivity, Density, and Viscosity Measurements

The functional properties of mucilage can be affected by its chemical composition. The mucilage densities at concentrations of 1, 4, and 6% are 1.03, 1.03, and 1.05 g·mL−1, respectively. These values are higher than those reported forO. ficus-indica (0.85 g·mL−1) andO. stricta (0.81 g·mL−1) at concentrations of 8% [1]. However, the density obtained for theO. cochenillifera mucilage is comparable to those reported for gum arabic (1.00–1.02 g mL−1) at the same concentrations [35]. Gum arabic is the most utilized type of gum in food and other industrial applications because of its good emulsifying and stabilizing properties.The conductivities of the obtained mucilage solutions are lower than those reported in the literature forO. ficus-indica but comparable toO. stricta[1]. The conductivity values for samples prepared at concentrations of 1, 4, and 6% are 2.3, 4.9, and 6.4 mS cm−1, respectively. Variations in the conductivity at different concentrations may be attributed to the presence of greater numbers of divalent and monovalent ions, which increase the conductivity, as has been reported for theO. ficus-indica mucilage [1]. According to Gebresamuel and Gebre-Mariam [1], the presence of electrolytes in the mucilage can be of value in the flocculation of suspension formulations.The pH measurements reveal that the mucilage at different concentrations is slightly acidic (4.8–5.0). This acidic nature indicates that the mucilage contains uronic acids in its structure. The pH values are lower than those found by Contreras-Padilla et al. [18] forO. ficus-indica (5.5–6) but comparable to those reported for gum arabic (4.5–5.6) [36, 37]. The pH is also a critical factor in coagulation/flocculation processes, wherein the optimal pH should be between 5 and 7.5 [38].The mucilage viscosities for solutions of 1 and 4% are 1.6 and 4.6 mPa·s, respectively. These values are comparable to those for 1 and 4% solutions of pure gum arabic (1.3 and 2.4 mPa·s, resp.) [35]. This ability of mucilage to form low viscosity solutions at low concentrations in the same manner as gum arabic should enable it to form solutions in a wide range of concentrations with excellent properties as an emulsifier and stabilizer.


#### 3.3.2. Water- and Oil-Holding Capacities

O. cochenillifera mucilage presents a better WHC (2.78 g water/g dry mucilage) than OHC (1.80 g oil/g dry mucilage). The WHC influences the formation of viscous solutions that can facilitate industrial processes. Mucilage forms a three-dimensional network in contact with water, trapping it and resulting in highly viscous solutions. Mucilage is primarily composed of galactose, mannose, xylose, and other sugars, and, thus, has a high capacity to bind or retain water, similarly to pectins, gums, and some algal polysaccharides. Because of this large water absorption capacity, mucilage may find applications in foods, cosmetics, and pharmaceuticals, in which it can dissolve, be dispersed, and form colloids [13]. Similarly, mucilage can be used to modify the rheological properties of soil, acting as a binding agent in soil aggregation [2, 12]. The OHC would allow its use in combination with other products to collect petroleum and various oils in case of spills on water. In addition, the good OHC value suggests that mucilage could improve the texture of food products.


### 3.4. Removal of Textile Dyes as a Sample Application

Mucilage has the potential to be used in the clarification of water due to its ability to retain different types of particles that are dispersed therein [9]. Additionally, as a negatively charged polyelectrolytic molecule due mainly to its sugar composition, mucilage has the ability to attract or retain certain types of positively charged substances. As demonstrated in this investigation, the capacity of theO. cochenillifera mucilage to remove textile dyes from aqueous solutions is considerable (Figures 4(a) and 4(b)). The removal percentage varied depending on the mucilage concentration and the dye, with maximum values of 73% and 49% for the green and blue dyes, respectively, at a concentration of 3% mucilage. These results agree with those reported by Peláez-Cid et al. [39] in which 5–95% of the textile dyes were removed from aqueous solutions usingO. ficus-indica fruit waste as an adsorbent. According to Anjaneyulu et al. [40] adsorption methods for the removal of dyes are based on the high affinity of the dyes. Adsorptive bleaching is influenced by several factors, such as the physicochemical dye-adsorbent interactions, adsorbent surface area, particle size, temperature, and contact time.Figure 4
Removal of textile dyes at different concentrations of mucilage: (a) green dye and (b) blue dye.
(a)
(b)O. cochenillifera mucilage can be considered a low-cost biosorbent and environmentally friendly alternative for water clarification. For example, the textile industry worldwide consumes tremendous amounts of water in dyeing processes, and wastewaters from this industry are some of the most polluted across all industrial sectors. Some dyes and byproducts are carcinogens or mutagens and aesthetically deteriorate water bodies and impact flora and fauna. Zhang et al. [41] compared the ability of a mucilage clarifier with other traditional agents such as aluminum sulfate, reporting that the mucilage ofO. ficus-indica demonstrated similar behavior to aluminum sulfate.


## 3.1. Mucilage Extraction

The mucilage yields obtained from fresh and dried cladodes using thermal extraction varied from 22 to 25% and 20 to 33% on a dry matter basis (Table2), respectively. From the experimental design data and mucilage percentage obtained under each condition (Table 4), quadratic polynomials were determined (see (1)) for the fresh and dried cladodes, respectively, and validated by the ANOVA test.(1)Mucilagefresh,%=22.0±0.3+0.3±0.2t+0.02±0.2T+0.7±0.2t2-0.7±0.3tT,Mucilagedried,%=21.3±1.5-2.1±1.3T+4.6±1.4T2,where t is time and T temperature.Table 2
Mucilage yields fromO. cochenillifera obtained via thermal extraction.
Experiment number
Yield
Yield
(%)a
(%)b
1
21.7
27.4
2
23.8
29.0
3
23.3
24.0
4
22.1
13.2
5
23.6
21.1
6
24.6
19.6
7
22.1
33.0
8
22.3
27.2
9
21.9
24.1
10
21.8
20.5
11
22.4
21.1
aFresh cladodes.
bDried cladodes.In the case of the fresh cladodes, the linear term for time has a positive coefficient, meaning that the mucilage extraction increases with time. The positive quadratic terms indicates that large variation of time in either direction will result in extraction yield increase (the response surface shows a minimum). However, the linear term for temperature has no effect on mucilage yield, but considering the confidence intervals, the interaction between both variables has a significant effect on mucilage extraction. For the dried cladodes, the linear term for the temperature has a negative coefficient, meaning that the extraction yield increased as the temperature declined. The positive quadratic terms indicates that large variation of temperature in either direction will result in extraction yield increase. Time appears to have no significant effect on mucilage extraction for the range studied (50–80 min). Considering the confidence intervals, the interactions between variables have no significant effect on mucilage extraction.Error values corresponded to a 95% confidence level. The effects of the extraction conditions on the mucilage yield are shown in the response surface graph for the polynomials (within the studied variable ranges) (Figures1(a) and 1(b)). The responses are close to the experimental values, with correlation coefficients (r2) of 0.93 and 0.89 for the fresh and dry cladodes, respectively.Figure 1
Response surfaces for removal of mucilage extracted fromO. cochenillifera: (a) fresh cladodes and (b) dry cladodes.
(a)
(b)The optimum values of the variables for the maximal mucilage yields were determined by the SIMPLEX method using the maximum values of the response surface. The maximum mucilage yields predicted for the fresh and dried cladodes are24.5±0.3% and 34±1%. The predicted values of the best extraction variables are 54 min and 80°C for the fresh cladodes and 86 min and 44°C for the dried cladodes. The experimental mucilage yields for the fresh and dried cladodes obtained under these conditions are 24±1% and 31±2%, respectively, which agree well with the predicted values. Mucilage extraction from the dried cladodes was better than from the fresh cladodes, which may be related to the larger surface area of the former, which would improve the extraction process.The nonthermal methods of extraction from the cladodes were based on hydration, agitation, and hydration and agitation processes. Table3 shows the mucilage yields obtained for the three approaches. Increased performance is observed for the samples subjected to the hydration and hydration/agitation processes, compared to agitation alone. This indicates that the hydration process is very important when mucilage extraction is performed with previously dried and powdered cladode samples. The results obtained were analyzed using ANOVA and Tukey’s HSD multiple comparison test (p≤0.05), which showed that there is a significant difference between the mean of the agitation process with the other two processes at the 95% confidence level.Table 3
Mucilage yields via nonthermal extraction fromO. cochenillifera cladodes.
Treatment
Yield (%)
Hydration
31 ± 1
Agitation
26.4 ± 0.1
Hydration and agitation
31 ± 2Table 4
Mineral content of mucilagefromO. cochenillifera.
N
P
K
Ca
Mg
%
1.6
0.4
1.2
1.8
0.3
Fe
Cu
Mn
Zn
Na
Mg·kg−1
191
424
344
386
250The maximum mucilage extraction yields obtained from cladodes under the thermal and nonthermal extraction methods in this study are similar and/or higher than those reported for otherOpuntia such asO. streptacantha (7.2%),O. megacantha (7.4%),O. albicarpa (6.9%),O. milpa alta (7%),O. dillenii(16%), andO. ficus-indica (4–25%) [8, 18–20].


## 3.2. Chemical Characterization of the Mucilage

The total carbohydrate content was 40%, which is higher than that reported forO. dillenii, with 12 to 15% as polysaccharides [20], but within the range given forO. ficus-indica (13–64%) [21, 22]. In addition, the mucilage is an excellent source of essential minerals such as calcium, phosphorus, magnesium, iron, potassium, zinc, and copper (Table 4). Calcium is the most abundant mineral in the mucilage, which agrees with other studies of cactus pads [23–25]. For example,O. ficus-indica was a better source of calcium than spinach, soy, and grains, suggesting thatOpuntia spp. may have potential in the prevention and treatment of diseases such as osteoporosis [26]. Because of their excellent nutritional qualities,Opuntia (especiallyO. indica) have been used as food sources in countries such as Mexico. As theO. cochenillifera mucilage is a rich source of carbohydrates and essential minerals, it has good potential for use as a nutritional supplement.The crude protein content was determined as 7.4%. This value is comparable to those reported forO. ficus-indica cladodes (5–9%) but higher than those inO. stricta (5%) and guar gum (3–5%) [1, 27, 28]. The interactions that occur through the specific (hydrophilic) functional groups of polysaccharides and proteins are an important factor in the study of mucilage proteins; these form a three-dimensional network that can improve the stability and uniformity of the system matrix and suggest potential application in the industry [29]. Usually, proteins and polysaccharides are safe food additives that can form physically stable emulsions [30].The phytochemical analysis shown in Table5 reveals the presence of alkaloids by the Dragendorff, Mayer, and Wagner tests, which identify quaternary alkaloids and/or amine-oxides. The TLC analysis also revealed the presence of alkaloids; two spots were visualized at 254 nm (Figure 2), using different mixtures of eluents. Ethyl acetate/methanol/chloroform/hexane (6 : 1 : 2 : 1) is the best eluent employed, showing Rf values 0.88 and 0.63, respectively (Table 6). Likewise, two spots were observed with Dragendorff and Wagner reagents. The presence of terpenes/steroids was also found using the Salkowski test. Although the presence of saponins, flavonoids, and tannins was not found in this study, Tomás Ch et al. [31] reported the presence of saponins, flavonoids, and alkaloids in the pulp ofO. ficus-indica. The chemical composition of theOpuntiaspp. is quite variable, depending on a number of factors such as the chemical characteristics of the soil, geographical location, environmental conditions, age, and species [8, 22, 27].Table 5
Phytochemical analysis ofO. cochenillifera mucilage.
Metabolite
Test
Mucilage
Alkaloids
Meyer
(+)
Dragendorff
(+)
Wagner
(+)
Saponins
Rosenthaler
(−)
Tannins
FeCl3
(−)
Terpenes/steroids
Salkowski
(+)
Flavonoids
Reaction with NaOH
(−)
Shinoda
(−)
5-hydroxy flavones
Dimroth
(−)Table 6
Alkaloids analysis ofO. cochenillifera mucilage by TLC.
Eluent
Number of spots detected
Rf 1
Rf 2
Observation
Chloroform/methanol (9 : 1)
2
0.70
0.93
Brown spots with Dragendorff and Wagner reagent; fluoresced violet light at 254 nm.
Chloroform (100%)
2
0.70
0.82
Ethyl acetate/methanol/chloroform/hexane (6 : 1 : 2 : 1)
2
0.63
0.88Figure 2
TLC based detection of alkaloids ofO. cochenillifera mucilage extracts visualized under UV at 254 nm.The FT-IR spectrum of the mucilage exhibits typical bands forOpuntiaspp. The functional group bands found in theO. cochenilliferamucilage (Figure 3) are characteristic for proteins and polysaccharides. The bands at 3420, 2931, and 1623 cm−1 represent the stretching vibrations of O–H, C–H, and –COO− (asymmetric vibrations) groups, respectively, in carbohydrate and uronic acid molecules. Further, the bands at 2931 and 1623 cm−1 appear to be associated with the N–H stretching and bending motions, respectively, of proteins. Han et al. [20] and Contreras-Padilla et al. [18] reported bands at 3500–3200 cm−1 corresponding to carbohydrate O–H bonds inO. dillenii andO. ficus-indicamucilage. Also, they assigned a band around 2920 cm−1 to the C–H stretching vibration of the pyranose group. Zhao et al. [32] attributed the bands at 1620, 1596, and 1420 cm−1 to deprotonated carboxylic acid groups (–COO−) in uronic acid inO. monacantha.Similar bands are observed at 1623, 1582, and 1431 cm−1 in our spectrum. The bands found at ~1431–1264 cm−1 can be assigned to C–O stretching and O–H deformation vibrations, according to Han et al. [20] and the bands at 1431–1393 cm−1 indicate C–N stretching modes [33]. The bands at 1085 and 1045 cm−1 indicate the presence of monosaccharides such as mannose and glucose in pyranose ring conformations [20, 34]. The absorption band at 893 cm−1 corresponds to β-d-glucose [32]. The bands at 774 and 608 cm−1 are attributed to N–H and O–H out-of-plane vibrations, respectively [32, 33].Figure 3
FT-IR spectrum ofO. cochenillifera mucilage.


## 3.3. Physical Characterization of the Mucilage

### 3.3.1. pH, Conductivity, Density, and Viscosity Measurements

The functional properties of mucilage can be affected by its chemical composition. The mucilage densities at concentrations of 1, 4, and 6% are 1.03, 1.03, and 1.05 g·mL−1, respectively. These values are higher than those reported forO. ficus-indica (0.85 g·mL−1) andO. stricta (0.81 g·mL−1) at concentrations of 8% [1]. However, the density obtained for theO. cochenillifera mucilage is comparable to those reported for gum arabic (1.00–1.02 g mL−1) at the same concentrations [35]. Gum arabic is the most utilized type of gum in food and other industrial applications because of its good emulsifying and stabilizing properties.The conductivities of the obtained mucilage solutions are lower than those reported in the literature forO. ficus-indica but comparable toO. stricta[1]. The conductivity values for samples prepared at concentrations of 1, 4, and 6% are 2.3, 4.9, and 6.4 mS cm−1, respectively. Variations in the conductivity at different concentrations may be attributed to the presence of greater numbers of divalent and monovalent ions, which increase the conductivity, as has been reported for theO. ficus-indica mucilage [1]. According to Gebresamuel and Gebre-Mariam [1], the presence of electrolytes in the mucilage can be of value in the flocculation of suspension formulations.The pH measurements reveal that the mucilage at different concentrations is slightly acidic (4.8–5.0). This acidic nature indicates that the mucilage contains uronic acids in its structure. The pH values are lower than those found by Contreras-Padilla et al. [18] forO. ficus-indica (5.5–6) but comparable to those reported for gum arabic (4.5–5.6) [36, 37]. The pH is also a critical factor in coagulation/flocculation processes, wherein the optimal pH should be between 5 and 7.5 [38].The mucilage viscosities for solutions of 1 and 4% are 1.6 and 4.6 mPa·s, respectively. These values are comparable to those for 1 and 4% solutions of pure gum arabic (1.3 and 2.4 mPa·s, resp.) [35]. This ability of mucilage to form low viscosity solutions at low concentrations in the same manner as gum arabic should enable it to form solutions in a wide range of concentrations with excellent properties as an emulsifier and stabilizer.


### 3.3.2. Water- and Oil-Holding Capacities

O. cochenillifera mucilage presents a better WHC (2.78 g water/g dry mucilage) than OHC (1.80 g oil/g dry mucilage). The WHC influences the formation of viscous solutions that can facilitate industrial processes. Mucilage forms a three-dimensional network in contact with water, trapping it and resulting in highly viscous solutions. Mucilage is primarily composed of galactose, mannose, xylose, and other sugars, and, thus, has a high capacity to bind or retain water, similarly to pectins, gums, and some algal polysaccharides. Because of this large water absorption capacity, mucilage may find applications in foods, cosmetics, and pharmaceuticals, in which it can dissolve, be dispersed, and form colloids [13]. Similarly, mucilage can be used to modify the rheological properties of soil, acting as a binding agent in soil aggregation [2, 12]. The OHC would allow its use in combination with other products to collect petroleum and various oils in case of spills on water. In addition, the good OHC value suggests that mucilage could improve the texture of food products.


## 3.3.1. pH, Conductivity, Density, and Viscosity Measurements

The functional properties of mucilage can be affected by its chemical composition. The mucilage densities at concentrations of 1, 4, and 6% are 1.03, 1.03, and 1.05 g·mL−1, respectively. These values are higher than those reported forO. ficus-indica (0.85 g·mL−1) andO. stricta (0.81 g·mL−1) at concentrations of 8% [1]. However, the density obtained for theO. cochenillifera mucilage is comparable to those reported for gum arabic (1.00–1.02 g mL−1) at the same concentrations [35]. Gum arabic is the most utilized type of gum in food and other industrial applications because of its good emulsifying and stabilizing properties.The conductivities of the obtained mucilage solutions are lower than those reported in the literature forO. ficus-indica but comparable toO. stricta[1]. The conductivity values for samples prepared at concentrations of 1, 4, and 6% are 2.3, 4.9, and 6.4 mS cm−1, respectively. Variations in the conductivity at different concentrations may be attributed to the presence of greater numbers of divalent and monovalent ions, which increase the conductivity, as has been reported for theO. ficus-indica mucilage [1]. According to Gebresamuel and Gebre-Mariam [1], the presence of electrolytes in the mucilage can be of value in the flocculation of suspension formulations.The pH measurements reveal that the mucilage at different concentrations is slightly acidic (4.8–5.0). This acidic nature indicates that the mucilage contains uronic acids in its structure. The pH values are lower than those found by Contreras-Padilla et al. [18] forO. ficus-indica (5.5–6) but comparable to those reported for gum arabic (4.5–5.6) [36, 37]. The pH is also a critical factor in coagulation/flocculation processes, wherein the optimal pH should be between 5 and 7.5 [38].The mucilage viscosities for solutions of 1 and 4% are 1.6 and 4.6 mPa·s, respectively. These values are comparable to those for 1 and 4% solutions of pure gum arabic (1.3 and 2.4 mPa·s, resp.) [35]. This ability of mucilage to form low viscosity solutions at low concentrations in the same manner as gum arabic should enable it to form solutions in a wide range of concentrations with excellent properties as an emulsifier and stabilizer.


## 3.3.2. Water- and Oil-Holding Capacities

O. cochenillifera mucilage presents a better WHC (2.78 g water/g dry mucilage) than OHC (1.80 g oil/g dry mucilage). The WHC influences the formation of viscous solutions that can facilitate industrial processes. Mucilage forms a three-dimensional network in contact with water, trapping it and resulting in highly viscous solutions. Mucilage is primarily composed of galactose, mannose, xylose, and other sugars, and, thus, has a high capacity to bind or retain water, similarly to pectins, gums, and some algal polysaccharides. Because of this large water absorption capacity, mucilage may find applications in foods, cosmetics, and pharmaceuticals, in which it can dissolve, be dispersed, and form colloids [13]. Similarly, mucilage can be used to modify the rheological properties of soil, acting as a binding agent in soil aggregation [2, 12]. The OHC would allow its use in combination with other products to collect petroleum and various oils in case of spills on water. In addition, the good OHC value suggests that mucilage could improve the texture of food products.


## 3.4. Removal of Textile Dyes as a Sample Application

Mucilage has the potential to be used in the clarification of water due to its ability to retain different types of particles that are dispersed therein [9]. Additionally, as a negatively charged polyelectrolytic molecule due mainly to its sugar composition, mucilage has the ability to attract or retain certain types of positively charged substances. As demonstrated in this investigation, the capacity of theO. cochenillifera mucilage to remove textile dyes from aqueous solutions is considerable (Figures 4(a) and 4(b)). The removal percentage varied depending on the mucilage concentration and the dye, with maximum values of 73% and 49% for the green and blue dyes, respectively, at a concentration of 3% mucilage. These results agree with those reported by Peláez-Cid et al. [39] in which 5–95% of the textile dyes were removed from aqueous solutions usingO. ficus-indica fruit waste as an adsorbent. According to Anjaneyulu et al. [40] adsorption methods for the removal of dyes are based on the high affinity of the dyes. Adsorptive bleaching is influenced by several factors, such as the physicochemical dye-adsorbent interactions, adsorbent surface area, particle size, temperature, and contact time.Figure 4
Removal of textile dyes at different concentrations of mucilage: (a) green dye and (b) blue dye.
(a)
(b)O. cochenillifera mucilage can be considered a low-cost biosorbent and environmentally friendly alternative for water clarification. For example, the textile industry worldwide consumes tremendous amounts of water in dyeing processes, and wastewaters from this industry are some of the most polluted across all industrial sectors. Some dyes and byproducts are carcinogens or mutagens and aesthetically deteriorate water bodies and impact flora and fauna. Zhang et al. [41] compared the ability of a mucilage clarifier with other traditional agents such as aluminum sulfate, reporting that the mucilage ofO. ficus-indica demonstrated similar behavior to aluminum sulfate.


## 4. Conclusion

O. cochenillifera mucilage is a functional plant-derived material that has potential applications in the pharmaceutical and chemical industries. It is a rich source of carbohydrates, proteins, and minerals and can be considered nontoxic and safe for humans. Indeed, several cultures have traditionally used the cladodes of theOpuntiaspp. as food. Its density, viscosity, pH, and conductivity characteristics recommend its use as an additive in the formulation of food and drugs.O. cochenilliferamucilage could be a good alternative emulsifier and stabilizing agent. Finally, the mucilage fromO. cochenillifera could be considered a natural technological alternative in many processes of decontamination for its ability to remove dyes.



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*Source: 4301901-2017-05-10.xml*