Novel Active Food Packaging Films Based on Whey Protein Incorporated with Seaweed Extract: Development, Characterization, and Application in Fresh Poultry Meat

Abstract

Algae and seaweeds are used in cookery since the beginnings of human civilization, particularly in several Asian cultures. Phenolic compounds are secondary metabolites produced by aquatic and terrestrial plants for their natural defense against external stimuli, which possess powerful antimicrobial and antioxidant properties that can be very important for the food industry. The main objective of this study was to develop a whey protein concentrate active coating, incorporated with a Fucus vesiculosus extract in order to delay the lipid oxidation of chicken breasts. Ten hydroethanolic extracts from F. vesiculosus were obtained and their antioxidant capacity was evaluated through two antioxidant activity assays: the DPPH radical scavenging activity and β-carotene bleaching assay. The total content in phenolics compounds was also determined by Folin-Ciocalteu method. The chosen extract was the one obtained from the freeze-dried F. vesiculosus using 75% (v/v) ethanol as extraction solvent. The extract was successfully incorporated into a whey protein film and successfully strengthened the thickness, tensile strength, and elastic modulus. The active film also was able to inhibit the chicken breasts lipid oxidation for 25 days of storage.

1. Introduction

Since the early stages of the human civilization, seaweeds are part of the traditional gastronomies of several Asian countries. Nutritionally, these type of plants are characterized for having a low fat content and a mineral content higher than the terrestrial plants, being a good matrix to be used for nutritional supplements in order to overcome some nutritional deficiencies [1,2,3,4]. Human consumption of seaweeds and algae is very common in the Asian culture, especially in Japan. In the Asian gastronomy, several species are consumed as seasonings and vegetables, which contribute for a diversification on their diet. On the other hand, recently, seaweeds and algae in Europe are used for supplementation or for industrial applications such as gelling agents [5,6].

Terrestrial and aquatic plants, for their defense against UV radication, pathogenic organisms, predators and parasites, naturally produce secondary metabolites known as phenolic compounds. These compounds are also responsible for the plants’ coloration and organoleptic properties [7,8,9,10,11]. Moreover, the bioactivity of plants, namely antioxidant and antimicrobial properties, are related to their content in phenolic compounds. The content in phenolic compounds depends on the plant’s edaphoclimatic characteristics, such as the soil, the geographical location, the moment of harvest, among others [10,12,13,14]. These active compounds can be obtained in the form of essential oil or extract through several extraction methods that can be applied to fresh, dried or freeze-dried plants and fruits.

Fucus vesiculosus is a brown edible seaweed (Class Phaeophyceae), known for its high iodine content and can be easily found in the tempered and cold zones of the North Atlantic [15,16,17]. The deficiency of iodine is a very serious issue once it can lead to serious conditions. Iodine is a micronutrient essential during the gestation period and for the proper functioning of the thyroid. This deficiency can cause neonatal death, decrease of intellectual development in children and can lead to infertility. The World Health Organization (WHO) recommends a diary intake of 150 µg/day for adults and 200–300 µg/day during the gestation period [18,19,20]. Although it is mainly under control in the first world countries, iodine deficiency still represents an important issue in undeveloped countries besides being the major preventable cause of brain damage in the world. In this vision, the WHO has set a goal to end iodine deficiency by 2020 [19,20]. Considering its high content in iodine and phytosterols, F. vesiculosus was recommended for obesity treatment. Although, this recommendation is no longer valid because of the secondary effects of iodine on the thyroid activity when treatment stops [21].

Food packaging main goal is to delay the foods’ natural degradation process, maintaining their organoleptic properties, protecting the packaged food during transportation and storage. With the advancement of technology, new packaging systems have emerged, such as active food packaging. This type of packaging, by direct interaction with the packaged food throughout the absortion or releasing systems, aims to prolong foods’ shelf-life maintaining or improving its organoleptic properties [22,23,24,25]. The releasing systems, as the name implies, release active compounds or substances to the packaged food with biological activities, such as antimicrobial or antioxidant [22,26]. Extracts and essential oils from aromatic plants, fruits by-products and seaweeds have powerful antioxidant activities due to their high content in phenolic compounds [27].

Till this day, lipid oxidation is one of the major causes of food spoilage and, consequently, originates high amount of food loss [28,29,30]. This natural occurring phenomenon can lead to molecular changes in foods, changes in foods’ nutritional value and formation of unpleasant tastes and/or aromas which, subsequently will reduce foods’ shelf-life [28,30,31]. Active food packaging incorporated with antioxidant substances can help to minimize this problem, which will gradually migrate to the food’ surface during storage time [31,32,33,34,35,36].

The objective of this study was to evaluate the antioxidant activity of ten hydroethanolic extracts obtained from F. vesiculosus L., and to incorporate the extract with the highest antioxidant capacity into a whey protein film as an active packaging to control lipid oxidation of chicken breasts.

2. Materials and Methods

2.1. Extract Production

F. vesiculosus was acquired from the Portuguese company, ALGAPlus™, Ílhavo, Portugal. The seaweed was washed three times in cold running tap water to removed most of the salt and possible impurities. One part of the seaweed was frozen and freeze-dried in a freeze drier (Heto PowerDry PL 9000, Thermo Fisher Scientific™, Waltham, MA, USA) and the other part was dried in an oven at 30 °C for 10 days, in the dark.

Five hydroethanolic solvents were used: 100% ethanol, 75% ethanol, 50% ethanol, 25% ethanol and 100% water. For the extraction process, the method described by Andrade et al. [37] was used. Briefly, to 5 g of the freeze-dried or the dried seaweed, 50 mL of solvent were added and homogenized for 30 min in a compact stirrer (Edmund Bühler™ Shaker KS 15 A, Hechingen, Germany) at 350 rpm. Then, the mixtures were centrifuged for 10 min at 2000 g (10,000 rpm) (Eppendorf AG 5804R, Hamburg, Germany). The supernatant was removed to an evaporation amber pear-shaped flask and ethanol was evaporated at 35 °C. The extracts with water were then frozen and freeze-dried.

2.2. Antioxidant Capacity Assays

For the antioxidant capacity assays, all the extracts were tested at 5 mg/mL with the exception of the 100% ethanolic extracts that were tested at 1 mg/mL due to their low yield (

Table 1. Seaweed extracts antioxidant properties characterization. Results are the means ± standard deviation of the replicants.

Solvent	Yield (%)		IP (%)		β-Carotene Assay (AAC)		TPC Assay (mg PGE/g of Extract)
	FD	D	FD	D	FD	F	FD	D
100% H20	18.63	26.66	62.51 ± 0.17 Ca	0.00 Cb	842.67 ± 5.55 Aa	575.10 ± 10.64 Bb	26.18 ± 0.11 Ea	19.03 ± 0.10 Cb
25% Ethanol	20.02	21.38	66.69 ± 0.33 Ba	17.88 ± 0.79 Bb	356.07 ± 6.42 Da	250.76 ± 5.31 Db	27.05 ± 0.31 Da	16.18 ± 0.09 Db
50% Ethanol	13.09	22.30	57.00 ± 0.47 Da	16.33 ± 0.86 Bb	564.59 ± 11.06 Ca	383.24 ± 7.07 Cb	31.12 ± 0.26 Ca	12.42 ± 0.11 Eb
75% Ethanol	4.71	18.77	78.26 ± 0.21 Aa	57.44 ± 0.99 Ab	636.22 ± 5.16 Ba	611.91 ± 8.09 Ab	45.21 ± 0.21 Ba	21.06 ± 0.12 Bb
100% Ethanol	2.71	3.86	44.65 ± 0.79 Ea	0.86 ± 0.03 Cb	237.82 ± 5.03 Ea	125.36 ± 11.90 Eb	194.65 ± 0.87 Aa	70.97 ± 0.74 Ab

Legend: FD–Freeze-dried; D–Dried; IP–Inhibition Percentage; AAC–Antioxidant Activity Coefficient; TPC-Total Phenolic Compounds; PGE–Phloroglucinol equivalents. (A−E): Within each parameter, values in the same column not sharing upper case superscript letters indicate statistically significant differences among solvents (p < 0.05); (a–b): Within each parameter, values in the same line not sharing lower case superscript letters indicate statistically significant differences among formulations (p < 0.05).

).

2.2.1. DPPH Radical Scavenging Assay

The antioxidant capacity of the ten hydroethanolic extracts was evaluated through the DPPH radical scavenging assay by the method described by Andrade et al. [37]. To 50 µL of sample, 2 mL of a methanolic solution of the DPPH radical (14.2 µg/mL) were added. The samples were homogenized and kept in the dark, for 30 min, at room temperature (23 ± 1 °C). The absorbance of the samples was measured at 515 nm in a Thermo Scientific Evolution 300 LC spectrophotometer. For the control samples 50 µL of the used solvent were used. The Inhibition Percentage (IP) was calculated by the Equation (1).

$$IP (\%) = \frac{AC-AS}{AC} \times 100$$

(1)

In which, AC stands for the absorbance of the control samples and the AS stands for the absorbance of the samples.

2.2.2. β-Carotene Bleaching Assay

The method applied in this study was initial described by Miller [38] and adapted by Andrade et al. [37]. To prepare the β-carotene and linoleic acid emulsion, 1 mL of a β-carotene in chloroform solution (2 mg/mL), 20 mg of linoleic acid and 200 mg of Tween^® 40 were mixed in an amber evaporation flask. Then, the chloroform was evaporated in a rotary evaporator at 40 °C, for 5 min, and 50 mL of ultra-pure water, obtained from a MilliQ™ filter system, were added and the solution was strongly shaken. Then, 5 mL of the emulsion were added to 200 μL of sample. For the control assays, 200 µL of solvent were used and the absorbance of the controls was measured at 470 nm. Then the controls and the samples were submitted at 50 °C for 2 h. At the end of this period, the absorbance of the samples and the controls were measured at 470 nm. The Antioxidant Activity Coefficient (AAC) was measured through the Equation (2).

$$AAC=\frac{AS-AC2}{AC0-AC2}\times 1000$$

(2)

wherein, AS stands for the absorbance of the sample, AC0 stands for the absorbance of the control before heating and AC2 stands for the absorbance of the control after heating.

2.3. Total Phenolic Compounds (TPC)

The total content on Phenolic Compounds was determined through the method described by Wang et al. [39]. Briefly, to 1 mL of sample, 5 mL of an aqueous solution of Folin-Ciocalteu (10%, v/v) was added. The mixture was homogenized and, after 5 min, 4 mL of an aqueous solution of sodium carbonate (7.5%, w/v) were added. The mixtures were homogenized and kept in the dark for 2 h, at room temperature (23 ± 1 °C). The samples absorbance was measured at 725 nm. The results are expressed in mg equivalents of phloroglucinol per g of extract.

2.4. Whey Protein Film Production

The active film was produced by casting, applying the method described by Andrade et al. [37] and is composed by 8% of concentrated whey protein, 8% of glycerol, 1% of F. vesiculosus L. extract and 83% of water. The whey protein concentrated was acquired from MyProtein^® (Chicago, IL, USA). Briefly, the whey protein was mixed with water using an Ultra-Turrax (IKA DI 25 basic, Werke GmbH & Co., Staufen im Breisgau, Germany) and then submitted to 80 °C for 30 min in a thermostatic bath. Then, the mixture was rapidly cooled in ice for 15 min. Glycerol and F. vesiculosus L. extract were added, homogenized with the Ultra-Turrax and casted in an aluminum foil surface. The film was left to dry for 3 to 4 days, at room temperature.

2.5. Film Mechanical Properties and Thickness

The films thicknesses was measured with a digital micrometer (0.001 mm, Mitutoyo, Japan) on ten randomly points of each sample, and the results were expressed by the means ± standard deviation.

The film mechanical properties (tensile strength, elastic modulus and elongation at break) were determined using the universal testing machine Shimadzu Autoghaph (Shimadzu, Australia), equipped with a 0.5 kN load cell, in accordance with ASTM D882–12 [40]. Five specimens of each repetition/treatment with dimensions of 150 × 25 mm² were evaluated using the grip separation speed of 50 mm/min and an initial gauge length of 50 mm. The mechanical parameters were calculated from the stress × strain curves, where the tensile strength (TS) corresponds to the maximum stress before breaking (i.e., the force divided by the area in which the traction is applied), the elastic modulus (EM) represents the slope of the straight-line portion of a stress-strain curve and the percentage of elongation at break (EAB) is the ratio between the stroke before breakage (maximum elongation) and the initial distance between grips [41].

2.6. Water Vapor Permeability (WVP)

Water vapor permeability (WVP) (mol/m·s·Pa) was obtained, at 30 °C, using the gravimetric method described by Ferreira et al. [42]. Samples of each film were sealed on top of glass cells (45 mm diameter) containing 8 mL of supersaturated NaCl solution (relative humidity (RH = 76.9%). The cells were then placed inside desiccators containing supersaturated CH₃COOK solution (RH = 22.5%) and equipped with a fan to promote air circulation and keep the driving force constant throughout the test. Prior to the test, the films were equilibrated in a desiccator containing supersaturated NaCl solution (RH = 76.9%) at 30 °C. The relative humidity and temperature of the inside air of the desiccators were monitored throughout the test using a thermo-hygrometer (Vaisala, Finland). The flow of water vapor was determined by weighing the cells at regular time intervals for approximately 22 h, and the WVP was calculated using Equation (3):

$$WVP=\frac{N_W\times \delta }{\Delta P_{w.eff}}$$

(3)

where Nw (mol/m²·s) corresponds to the flow of water vapor, δ (m) to the thickness of the film and ΔPw.eff (Pa) to the effective driving force. The results were expressed as the mean ± standard deviation of three replicates.

2.7. Film Optical Properties

The optical properties were evaluated by measuring the CIELab parameters L, a*, b*, using the Konica Minolta colorimeter (CR 400/410, Tokyo, Japan) with D 65 light source, and 10° visual angle. The analysis was conducted according to the CIELab color scale, where L is the measure of luminosity, ranging from zero (black) to 100 (white); a* the chromaticity of green (−60) to red (+60); and b* the chromaticity of blue (−60) to yellow (+60). From the L, a* and b* coordinates, the hue angle (hue*) and chromaticity were calculated using Equations (4) and (5) respectively.

$$hu{e}^{*} = arctan \left(\frac{b^{*}}{a^{*}}\right)\times \frac{180}{\pi }+180 , if a^{*} < 0$$

(4)

$$chromaticity = {\left(a^{*2}+ b^{*2}\right)}^{1/2}$$

(5)

2.8. Evaluation of the Lipid Oxidation

The chosen model food for the evaluation of the efficacy of the active package against lipid oxidation was chicken breast, which were kindly supplied by the Portuguese company, Lusiaves^® (Leiria, Portugal). The chicken breasts were packaged with the control (without the extract) and the active films, respectively, and stored at 4 ± 1 °C. To maximize the contact surface between the chicken breast and the active package, the samples were vacuum packaged (Figure 1). The chicken breasts were analyzed at the end of 3, 6, 8, 11, 15, 21 and 25 days of storage.

Thiobarbituric Reactive Substances Assay (TBARS)

The TBARS assay was performed according to the method described by Rosmini et al. [43] with minor changes. In brief, 10 g of minced chicken breasts were mixed with 20 mL of trichloroacetic acid (7.5%, w/v) and homogenized in a compact stirrer at 400–450 rpm. After 1 h, the solutions were filtered through a Whatman n° 1 paper filter. Then, 5 mL of the filtered samples were mixed with 5 mL of an aqueous solution of thiobarbituric acid (2.88 mg/mL, w/v). The solutions were homogenized and submitted to 95 °C for 30 min. Then, they were rapidly cooled in ice for 15 min and their absorbance was measured at 530 nm. The results are present in mg of malonaldehyde equivalents per kg of meat.

2.9. Statistical Analysis

All experiments were conducted using three replications. Statistical analysis of data was performed through a one-way analysis of variance (ANOVA) using the Software OriginLab, version 8.5 (OriginLab Corporation, Northampton, USA). The differences among mean values were processed by the Tukey test. All requirements necessary to carry out the ANOVA (namely, normality of data and homogeneity of variances) have been validated. Significance was defined at p < 0.05. Results are expressed as the means of the replicants ± standard deviation.

3. Results

3.1. Antioxidant Assays

The results of the antioxidant assays can be observed in Table 1. All the obtained extracts from the freeze-dried seaweed presented a significantly better antioxidant capacity results than the extracts obtained from the dried seaweed, probably because the freeze-drying process protected the seaweed bioactive compounds [44,45].

As expected, the extracts obtained with a higher ethanol percentage, presented the lowest yields. Additionally, the extracts obtained from the dried seaweed, presented higher yields than the extracts obtained from the freeze-dried seaweeds. The extract obtained with the 75% ethanol presented the highest inhibition of the DPPH radical percentage, followed by the extract obtained with 25% ethanol. On the β-Carotene Bleaching Assay, the 100% aqueous extract presented the highest antioxidant activity coefficient, followed by the 75% ethanol extract. Regarding the total phenolic compounds content, the value obtained for the 100% ethanol extract was the highest, followed by the extract obtained by ethanol at 75%.

Based on extraction yields and antioxidant assays results, the extract obtained from the freeze-dried F. vesiculosus L. with 75% ethanol was chosen to be incorporated into the whey protein concentrate film.

3.2. Active Whey Protein Film

The control and the active film can be observed above a paper sheet with the National Institute of Health Doutor Ricardo Jorge logo and applied to the chicken breasts (Figure 1).

3.2.1. Thickness, Mechanical Properties, Optical Properties and WVP

The addition of the F. vesiculosus extract seems to significantly increase the thickness of the control film in, approximately, 12% (p < 0.05), which is coherent with the greater solid content per surface unit (

Table 2. Film characterization. Results are the means ± standard deviation of the replicants.

Parameter	Control Film	Active Film
Thickness (μm)	248.8 ± 6.7 sig **	280.7 ± 7.5 sig
Tensile strength (MPa)	0.184 ± 0.022 ns	0.203 ± 0.055 ns
Elongation at break (%)	11.7 ± 2.5 ns	8.7 ± 1.9 ns
Elastic Modulus (MPa)	1.468 ± 0.617 ns	3.364 ± 1.300 ns
WVP (10−10 mol/m·s·Pa)	1.178 ± 0.21	Sample collapsed
L* (lightness)	84.51 ± 0.35 sig	60.72 ± 0.19 sig
a* [red (+a) or green (−a)]	−2.89 ± 0.02 sig	−1.33 ± 0.02 sig
b* [yellow (+b) or blue (−b)]	13.14 ± 0.66 sig	23.50 ± 0.03 sig
Hue*	102.42 ± 0.67 sig	93.25 ± 0.05 sig
Chromaticity	13.46 ± 0.64 sig	23.54 ± 0.03 sig

** Means followed by sig superscripts are statistically significant different (p < 0.05); ns (not significant).

). Regarding the other parameters, there were no significant differences, nevertheless, the addition of the F. vesiculosus extract seems to slightly reinforce some of the film’ physical properties. When compared to the control film (Table 2), the active film presented a higher value of tensile strength and elastic modulus which, in consequence, decreased the elongation at break (elasticity of the film). However, the extract addition seemed to increase the WVP of the film, since the active film collapsed in the first hours of the essay, which indicates that the extract addition made the films more hydrophilic. Fernandes et al. (2020) [46] also found a similar WVP value for a whey protein film with 30% of glycerol. The addition of glycerol appears to increase the WVP of whey protein films. Ribeiro-Santos et al. (2018) [26] used the same percentage of glycerol and found similar results for the control film. Once the samples with seaweed extract collapsed during the test, it is impossible to conclude whether it enhanced or diminished the film’s WVP, however as previously mentioned it probably enhanced the WVP, which corroborates with observed in Ribeiro-Santos et al. (2018) with the incorporation of a mixture of essential oils to whey protein films [26]. Gounga et al. (2007) [47] studied the influence of different whey protein and glycerol ratios on films’ WVP. The authors concluded that a higher percentage of whey protein increase the WVP and also, the higher the glycerol percentage (plasticizing effect), the higher the WVP [47].

Comparing with the results obtained by Ribeiro-Santos et al. (2018) [26], the whey protein film presented the same behavior, in terms of thickness and elongation at break, in the presence of an additive. In both studies, the addition of extract and essential oils seemed to thicken the film, as well as increase the tensile strength. Abdalrazeq et al. (2019) [48] studied the application of different percentages (40 and 50%, w/w) of glycerol into isolated whey protein based films. These films showed a higher tensile strength and were less thick than the control film in the present study, which can be explained by the higher percentage of added glycerol. Moreover, the elongation at break was higher in the film with 50% of glycerol and higher than the values found for the control and active films conceived in this study. However, the film with 40% of glycerol showed a lower elongation at break value (3.6%) than the control film [48] (Table 2).

The produced films were predominant yellowish, and the incorporation of the best active extract interfered on this optical parameter, which can be visually observed (Figure 2) and confirmed by the measured CIELab coordinates (Table 2). Films incorporated with the extract got darker (increased L, p < 0.05) with a stronger yellow appearance (higher b*, p < 0.05). A similar behavior was also observed in chitosan films incorporated with hydroalcoholic extracts from different plants (food seasoning herbs and tea) [49] or essential oil [50]. The extracts contribute to add color to the films due to their intrinsic color, and the ability of their active compounds to structurally bind with the polymer, changing the film’s optical properties [49]. The active film presented a hue angle around 90°, which corresponds to the yellow color. On the other hand, the control films presented a superior angle (around 102·), which indicates a tendency to the green color (Table 2). These results suggest that the extract potentialize the yellow color in the active films when compared to the control films. Regarding the chromaticity, the extract significantly (p < 0.05) increased the films’ color saturation, which means that the active film present more vivid colors than the control film [49]. The optical values of the control film were higher than the values of the whey protein film produced by Ribeiro-Santos et al. [26], indicating that the film produced in this study was more shining (L), green (−a) and yellow (+b).

3.2.2. TBARS Assay

Lipid oxidation is a natural complex phenomenon. Its initiated by the formation of free peroxyl radicals, which will react with unsaturated fatty acids, forming lipid hydroperoxides. Antioxidant compounds may inhibit lipid oxidation of the unsaturated fats by prevent the formation of free peroxyl radicals and the formation of lipid hydroperoxides [51,52,53].

The TBARS assay is one of the most common methods to evaluate foods’ lipid oxidation by measuring the malonaldehyde (MDA) content. MDA is an aldehyde formed during the polyunsaturated fatty acids peroxidation, being a product of the primary oxidation of lipids [32,52,53,54]. However, this assay only measures substances reactive to the thiobarbituric acid which, during lipid oxidation, will continue to be degraded [32,55]. The results of the TBARS assay are present in Figure 2. For this assay, a calibration curve (y = 308.7x − 0.0071) was obtained using 1,1,3,3-tetramethoxypropane as standard. The determination coefficient of the calibration curve was 0.9995, in a working range of 0.1–3 μg/mL, indicating linearity and correlation. As can be observed in Figure 2, the chicken packaged with the active film for 15, 21 and 25 days of storage, presented a significantly lower MDA value than the chicken packaged with the control film. The decrease of the MDA content on the 8th day of storage seems to suggest that the oxidative status of the chicken breasts reached an oxidation peak between the 6th and the 8th day of storage. Shahbazi and Shavisi [56] also registered the same TBARS behaviour in rainbow trout fillets on the 10th day of storage. This can also be explained by the chemical reactions between MDA and the meat compounds, which may lead to a decrease in the MDA amount [56,57].

Although not conclusively, the study lead by Reboleira et al. [58] showed some inhibition of chicken patties’ lipid oxidation when in contact with Porphyra dioica extract for 96 h (4 days). Gonçalves et al. [59] evaluated the effect of microalgae biopeptides nanofibers in chicken breasts. The authors found that the chicken with the microalgae nanofibers presented a lower MDA value (1.0 ± 0.0 mg MDA/kg) than the control breast chicken (2.6 ± 0.0 mg MDA/kg). The values found in the study of Gonçalves et al. [59] are much higher than the values calculated for the chicken packaging with the whey protein film. The authors studied the influence of polycaprolactone (PCL) nanofibers incorporated with microalgae biopeptides on chicken lipid oxidation. At the end of 12 days of storage, the MDA values were much higher than the values found in this study. However, the MDA content of the chicken meat at day 0 was also higher that the MDA value of the chicken breasts, indicating that the chicken evaluated on this study was ‘fresher’ [59].

4. Conclusions

A whey protein edible film incorporated with an ethanolic extract of Fucus vesiculosus L. was successfully prepared by casting method. The addition of the F. vesiculosus extract seems to reinforce some of the whey protein film physical characteristics, such as thickness, tensile strength, and elastic modulus. However, the addition of the extract made the film more permeable to water vapor. The new film was able to inhibit lipid oxidation of packaged poultry meat, at least for 25 days of storage compared with the control whey protein film. One of the studies limitations was the inability to perform other lipid oxidation assays, such as the determination and quantification of the aldehyde hexanal, responsible for the rancid smell and taste. The determination of the peroxide value is also another lipid oxidation evaluation assay, but the authors were not able to perform this assay in the laboratory. Moreover, the obtained results encourage more assays, namely microbiological assays, and sensorial analysis, in order to evaluate the effect of this new film in the extension of poultry meat shelf-life.