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Article

Electrospun Fibers of Ecovio® Polymer Blends with Antimicrobial Tea Tree Essential Oil: Enhanced Chemical and Biological Properties

by
Bianca Z. de Souza
1,
Débora P. Facchi
2,
Suelen P. Facchi
3,
Carlos F. Teodoro
2,
Débora A. de Almeida
2,
Ketul C. Popat
4,5,
Matt J. Kipper
6,
Elton G. Bonafé
1 and
Alessandro F. Martins
1,2,7,*
1
Laboratory of Materials, Macromolecules and Composites, Federal University of Technology—Pararná (UTFPR), Apucarana 86812-460, PR, Brazil
2
Department of Chemistry, State University of Maringá (UEM), Maringá 87020-900, PR, Brazil
3
Graduate Program in Agronomy, State University of Maringá (UEM), Maringá 87020-900, PR, Brazil
4
Department of Bioengineering, George Mason University (GMU), Fairfax, VA 22030, USA
5
Department of Mechanical Engineering, Colorado State University (CSU), Fort Collins, CO 80523, USA
6
Department of Chemical and Biological Engineering, Colorado State University (CSU), Fort Collins, CO 80523, USA
7
Department of Chemistry, Pittsburg State University (PSU), Pittsburg, KS 66762, USA
*
Author to whom correspondence should be addressed.
Processes 2024, 12(11), 2330; https://doi.org/10.3390/pr12112330
Submission received: 29 June 2024 / Revised: 21 October 2024 / Accepted: 21 October 2024 / Published: 24 October 2024
(This article belongs to the Special Issue Antimicrobials in Plants: From Traditional Medicine to Modern Therapeutic Agents)
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Abstract

:
This study presents the development of fibers with favorable properties for biodegradable wound dressings made from the Ecovio® (EC) polymer blend, composed of poly(lactic acid) (PLA) and poly(butylene adipate-co-terephthalate) (PBAT), incorporated with tea tree essential oil (TTE). TTE presented antimicrobial activity against Pseudomonas aeruginosa and Staphylococcus aureus, achieving minimal inhibitory concentrations (MIC) of 15 and 7.5 mg/mL, respectively. The TTE was mixed with EC in a binary chloroform and formic acid (85/15 v/v) mixture. The EC/TTE fibers were characterized by differential scanning calorimetry (DSC), Fourier-transform infrared with attenuated total reflectance (FTIR-ATR), and X-ray photoelectron spectroscopy (XPS), confirming the TTE in the fibers. The tests showed that TTE (0.5, 1.0, or 1.5 mL) improved the polymer blend’s electrospinnability, leading to bead-free, homogenous, and smaller fiber diameters. TTE (1.5 mL or 75 w% concerning the EC) leads to homogeneous fibers with an average diameter of 278 ± 59 nm. TTE (75 w%) increased the wettability of the EC fibers from 120 ± 2° to 69 ± 1°. Preliminary bacterial adhesion and proliferation assays demonstrated that the EC/TTE fibers have anti-adhesive activity and demonstrate greater toxicity, which seems more toxic against P. aeruginosa than S. aureus after 24 h of incubation. Fluorescence and coagulation kinetics tests performed with human blood indicated that the EC/TTE fibers accelerate blood coagulation. The EC/TTE fibers exhibit promising chemical and biological properties (in vitro) for developing wound dressings.

1. Introduction

Essential oils are typically found in plants but can also be synthesized by bacteria and insects [1]. They consist mainly of terpenoids but may include oxygenated compounds such as alcohols, ketones, aldehydes, esters, and phenolics [2]. These compounds possess unique biological properties, such as boosting the immune system, providing aromatherapeutic benefits that promote emotional well-being when diffused [3], and exhibiting anti-inflammatory [4,5], analgesic [6], antioxidant [4,5,7], antifungal [3], and bactericidal [3,8] activities.
Among various essential oils, tea tree essential oil (TTE) or Melaleuca alternifolia essential oil, has gained significant attention primarily due to its antimicrobial, anti-inflammatory, and wound-healing properties [9]. Melaleuca alternifolia, commonly known as the tea tree, is a member of the Myrtaceae family and is native to Australia and the Indian Ocean islands [10,11]. The primary product extracted from this plant is TTE, which has a yellowish color and distinctive odor. Australian Aboriginals have used this oil for thousands of years for its bactericidal and antifungal effects [12].
Clinical studies have shown that TTE promotes rapid wound healing [10,11]. In one study, wounds in 10 patients healed faster when treated with TTE than when treated with treatment that did not use the essential oil. The results demonstrated a significantly reduced healing time for all participants treated with TTE [9,13]. The oil’s wound-healing properties are primarily attributed to its anti-inflammatory, antioxidant, and antimicrobial capabilities [9]. It is recommended for treating skin lesions, insect bites, burns, acne, and nail fungal infections [14].
TTE is a complex mixture of many compounds with around 100 components. The primary constituents include terpinen-4-ol, γ-terpinene, and α-terpinene [12,14,15]. Terpinen-4-ol is the major component and is used for treating skin blemishes and relaxing muscles and joints. For TTE to exhibit antiseptic activity, the Australian committee stipulates that its composition should contain less than 15% cineole and more than 30% terpinen-4-ol [16]. Terpinen-4-ol, which constitutes 30–40% of the oil, is responsible for its antimicrobial activity by damaging the bacterial cell membrane [12].
However, the direct topical use of TTE has some disadvantages. When applied to the skin, it can cause contact dermatitis (an allergic skin rash), erythema, erythema multiforme-like eruption, linear IgA bullous disease, systemic hypersensitivity reactions, and anaphylaxis [17,18,19]. Its high commercial value poses a challenge, as approximately 300 kg of plant leaves are required to produce just 1 L of the oil. Incorporating TTE into polymeric materials can help mitigate or even prevent contact dermatitis and other side effects promoted by the topical application of the TTE [20]. The development of materials incorporated with TTE, such as films with poly(lactic acid) (PLA) [20] and electrospun fibers with poly(vinyl pyrrolidone) [21], are highlighted. These materials can retain the excellent biological properties (e.g., antimicrobial and anti-inflammatory activities [20,21]) of the TTE while reducing side effects by avoiding its direct topical application.
To produce fibers, the electrospinning technique has garnered significant interest from researchers in the fields of tissue engineering, biomedicine, pharmaceuticals, and functional materials. This is due to its ability to produce fibers with a high surface area-to-volume ratio and average diameters in the submicrometric and nanometric range [22,23,24,25]. These fibers can be used in tissue engineering, primarily for wound protection (wound dressings) and tissue repair (scaffolds), as they mimic the properties of some native tissues and organs that present fibrillar proteins, like collagen and elastin [26,27].
Wound dressings aid in the healing process without necessarily accelerating it. They play a crucial role in maintaining homeostasis, preventing bleeding, removing excess exudates, and protecting the wound against bacteria [28]. Wound dressings should not interact directly with the wound site and must be easily removable to prevent further damage. Their primary function is to shield the wound from external agents and contamination, promoting oxygenation, exudate removal, blood coagulation, and inhibiting bacterial adhesion and proliferation. Unlike scaffolds, wound dressings must be periodically replaced on the injured area [29,30,31,32].
In this context, the commercial and biodegradable blended Ecovio® (EC) fiber shows great potential for such applications, although it does not have antimicrobial activity [33,34,35]. EC is compostable and composed of hydrophobic and biodegradable polyesters, including PLA and poly(butylene adipate-co-terephthalate) (PBAT) [34,36]. Currently, BASF manufactures plastic materials based on the EC blend for use in organic waste packaging, sutures, and prostheses [37].
Therefore, this study aims to prepare, characterize, and evaluate the biological properties of EC fibers containing TTE, including antimicrobial activity and interaction with human blood. The EC fibers were prepared with different concentrations of TTE in a chloroform and formic acid (85/15 v/v) mixture. EC/TTE fibers were characterized by scanning electron microscopy (SEM), X-ray photoelectron spectroscopy (XPS), contact angle measurements, mechanical properties, and differential scanning calorimetry (DSC). Adhesion and proliferation assays of Pseudomonas aeruginosa (P. aeruginosa) and Staphylococcus aureus (S. aureus) indicated that the fibers possess antimicrobial activity primarily against P. aeruginosa. This study demonstrates for the first time that TTE incorporated into EC fibers can induce blood coagulation within just 15 min of contact due to interactions with platelets. These properties make EC/TTE fibers promising candidates for evaluation as protective agents (wound dressings) for skin wounds, as they can prevent prolonged bleeding and protect the wounds against bacterial deposition and proliferation.

2. Materials and Methods

2.1. Materials

The commercial Ecovio® (EC) blend (C2224F), composed of 55% poly(butylene adipate-co-terephthalate) (PBAT) and 45% poly(lactic acid) (PLA), was generously donated by BASF (São Paulo, Brazil). The solvents chloroform (99%) and formic acid (98%) were purchased from Sigma-Aldrich (São Paulo, Brazil). Tea tree essential oil (TTE), with a density of 0.8818 g/mL, was obtained from dōTERRA do Brasil Ltda (Joinville, SC, Brazil). Its chemical composition includes terpinen-4-ol (20–60%), terpinene (up to 55%), and alpha-pinene (1–10%)

2.2. Electrospun Solutions, Electrospinning, and Fiber Preparation

The fibers were prepared following the experimental procedure reported in the literature [34] with modifications. The conventional electrospinning method was used, and the electrospinning process was carried out in a horizontal position. EC solutions (5 mL) were obtained in a chloroform/formic acid mixture (85/15 v/v) at 23 °C. The TTE was added to the pre-prepared EC solution and thoroughly mixed by magnetic stirring. Table 1 presents the chemical composition of the electrospun solutions.
Before electrospinning, the solutions’ surface tension, electrical conductivity, and viscosity were investigated. Surface tension was measured using a Lecomte Du Nouy K6 tensiometer (KRÜSS, Heidelberg, Germany) at 25 °C, employing the Du Nouy method. The electrical conductivity of the solutions was estimated using a benchtop conductivity meter Mca-150, model MS Tecnopon at 25 °C (São Paulo, Brazil). The apparent viscosity of the solutions was determined using a Ubbelohde viscometer (São Paulo, Brazil) at 25 °C [34].
The EC and EC/TTE solutions were electrospun at a voltage of 12 kV, with a flow rate of 0.5 mL/h using an infusion pump (Harvard 2.2.2, Holliston, MA, USA). A copper plate covered with aluminum foil was used as a static collector. The solutions were electrospun with a 10 mL syringe connected to a stainless-steel capillary needle (14 G; 2.1 × 40 mm) at a distance of 10 cm from the metallic collector. The produced fibers were labeled EC/TTEx, where x represents the volume of TTE added to the EC solution (Table 1).

2.3. Fiber Characterization

The morphology of the fibers was analyzed using scanning electron microscopy (SEM) with a Thermo Fischer Scientific/Philips Quanta 250 apparatus (Prague, Czech Republic). The samples were coated with a gold layer of approximately 10 nm using cathodic spraying to enable electrical conduction. Contact angle measurements on the fiber surface were performed using the sessile drop method with Tantec A/S equipment (Lunderskov, Denmark). The fibers were characterized by differential scanning calorimetry (DSC) using a DSC-60 Plus instrument (Kyoto, Japan) under an argon atmosphere (50 mL/h) at a heating rate of 10 °C/min over a temperature range of 25 to 300 °C. Infrared spectra in the attenuated total reflection mode (FTIR-ATR), ranging from 2000 to 650 cm−1, were obtained using a Shimadzu Scientific instrument, model 8300 (Kyoto, Japan), with an acquisition rate of 64 scans/min and a resolution of 4 cm−1 [27].
The chemical composition of the electrospun fiber surface was evaluated using X-ray photoelectron spectroscopy (XPS) with a Phi Electronics 5800 spectrometer (Chanhassen, MN, USA) equipped with a hemispherical analyzer and a multichannel detector. Spectra were obtained using a monochromatic Al Kα X-ray source (hν = 1486.6 eV). An energy analyzer with a pass energy of 23.5 eV and steps of 0.10 eV was used, with an X-ray spot size of 800 μm. All spectra were collected with a photoelectron take-off angle of 45°. Gaussian peaks were fitted according to the expected functional groups [38].
The mechanical properties of the fibers were evaluated according to ASTM D882-10 specifications. Measurements were performed using a MicroSystems texture analyzer (Surrey, England) on samples measuring 50 × 10 mm with an average thickness of 0.014 ± 0.001 mm (n = 10). The initial distance set on the instrument was 30 mm, with a crosshead speed of 0.083 mm/s, and 5 kg load cells were used [27].

2.4. Antimicrobial Assay with the Tea Tree Essential Oil and Fibers

The minimal inhibitory and bactericidal concentrations (MIC and MBC) of TTE oil were evaluated against S. aureus (ATCC® 25923) and P. aeruginosa (ATCC® 27853) bacteria using the microdilution method as reported by Balouiri et al. [39] with alterations. Suspensions (200 μL) of bacteria at 1.0 × 107 CFU/mL were placed in contact with the essential oil in a 48-well microdilution plate containing 200 μL of Mueller–Hinton culture medium (pH 7.4 ± 0.2). The plate was then incubated for 24 h at 37 °C.
MIC is defined as the lowest concentration that inhibits bacterial growth. For MIC determination, after 24 h of contact between the microbial suspension and TTE oil, 10 μL of a resazurin solution (0.1% w/v) was added to each well. The pink coloration of resazurin indicates high cellular activity and viability. Conversely, the blue coloration of the dye indicates microbial growth inhibition. Thus, MIC is estimated based on a colorimetric test, as reported elsewhere [40]. After 1 h of contact with the resazurin dye, 10 μL of suspension from wells with blue coloration indicating microbial growth inhibition was collected. These aliquots were seeded onto Petri dishes containing Mueller–Hinton agar for 24 h at 37 °C to estimate the MBC, which is the lowest concentration that eliminates bacteria (99.99% or more) and prevents colony-forming units (CFUs) on Petri dishes. Control tests were also conducted. The positive control test involved adding 10 μL of microbial suspension (107 CFU/mL) without TTE oil presence to the Petri dish on Mueller–Hinton agar for 24 h at 37 °C. The negative test was performed by adding 10 μL of liquid culture medium in the presence of TTE oil but without bacteria on the Petri dish and Mueller–Hinton agar for 24 h at 37 °C.
The antimicrobial activity of EC/TTE fibers was assessed using the disk diffusion method on the Muller–Hinton agar medium [41]. This method aimed to evaluate the diffusion capability of TTE within the microbial culture plate and the potential formation of inhibition zones against S. aureus (ATCC® 25923) and P. aeruginosa (ATCC® 27853) bacteria [42,43]. Before the antimicrobial assays, the fibers (disks of 6 mm in diameter) were sterilized with ethylene oxide at 40 °C for 120 min (G&S Sterilization of Health Products, Brazil) [35].
Bacteria were suspended in saline solution (0.9% w/v) and spread onto Muller–Hinton agar plates in Petri dishes (90 × 15 mm). Filter paper disks impregnated with TTE (10 μL) and EC/TTE fibers (6 mm diameter disks) were placed on the plates containing the bacteria. The plates were then incubated at 37 °C for 24 h. After incubation, the diameters (mm) of the inhibition zones formed around the disks were evaluated. A control assay was conducted using filter paper disks impregnated with TTE.

2.5. Anti-Adhesive Assay with Bacteria

The anti-adhesive properties of the fiber surfaces were evaluated according to Plath et al. [27] with alterations. Before the assay, fiber disks (6 mm in diameter) were attached to the polystyrene disks (6 mm) using a double-sided tape. The prepared samples were sterilized with ethylene oxide at 40 °C for 120 min (G&S Sterilization of Health Products, Brazil) [35].
The anti-adhesive properties of EC, EC/TTE0.5, EC/TTE1.0, and EC/TTE1.5 fiber surfaces were analyzed, and the results were compared with a negative control based on polystyrene disks (6 mm). Bacterial suspensions (500 μL) in Mueller–Hinton medium were inoculated onto the samples in a 48-well plate at 1.0 × 107 CFU/mL for 24 h (n = 3). After incubation, the microbial suspension was removed, and the surfaces were washed once with PBS. The bacteria on the samples were fixed for SEM visualization using a solution containing 3% v/v glutaraldehyde (Sigma-Aldrich, São Paulo, Brazil), sodium cacodylate (0.1 M; Sigma-Aldrich, São Paulo, Brazil), and sucrose (0.1 M; Sigma-Aldrich, São Paulo, Brazil) for 45 min at room temperature. Subsequently, the samples were washed with 0.1 M sodium cacodylate and 0.1 M sucrose solution for 10 min each, followed by rinsing in water for 10 min. After removing the rinse water, the samples were freeze-dried for 24 h, then gold-coated and imaged by SEM at an acceleration voltage of 10–20 kV.

2.6. Platelet Adhesion Assay

Whole blood was obtained from a healthy individual following a protocol approved by the Institutional Review Board of Colorado State University. The blood was collected in 10 mL EDTA-coated tubes (BD). Plasma, containing platelets and leukocytes, was separated by centrifugation at 100× g for 15 min to remove red blood cells. Platelets and leukocytes were allowed to rest for 10 min before use. The plasma and cells were combined in a sterilized 50 mL conical tube. The sterilized samples (6 mm disks fixed on polystyrene disks) were placed in a 24-well plate and incubated with 200 μL of plasma for 2 h at 37 °C and 5% CO2 at 100 rpm. After incubation, the plasma was aspirated, and the samples were washed with PBS to remove non-adherent platelets from the fiber surfaces. Subsequently, a 2.0 μM calcein–AM solution in PBS was added to the samples and incubated for 30 min on an orbital shaker at room temperature. The solution was then aspirated, and the surfaces were washed with PBS three times. Platelet adhesion on the fiber surfaces was examined using fluorescence microscopy with a Zeiss Axiovision microscope (Dublin, OH, USA). The assay was conducted in triplicate, with 10 fluorescence images captured in each replicate. Image analysis was performed using ImageJ Software (version 1.53, Bethesda, MD, USA) to quantify the percentage of surface area covered by adhered platelets [44].

2.7. Whole Blood Coagulation Assay

To assess human blood clotting in the presence of fibers, sterilized samples (6 mm) were incubated with fresh blood (as-obtained from the donors) in a 24-well plate. A 7.0 μL drop of human blood was added to each fiber sample and left for 15 min. After incubation, the fibers were removed and transferred to another 24-well plate containing 500 μL of deionized water. The samples were agitated for 5 min on a horizontal shaker to release free hemoglobin and disperse non-coagulated blood cells. Subsequently, the absorbance of the free hemoglobin was measured at 540 nm using a plate reader (FLUOstar Omega, BMG LABTECH, Cary, NC, USA).

2.8. Statistical Analysis

At least three different examples of each sample were used in all experiments; the results are presented as mean ± standard deviation. Differences were determined using one-way ANOVA (p = 0.05) with a post hoc Tukey’s honest significant difference test.

3. Results and Discussion

3.1. Solution Properties

The TTE dissolves in the EC solutions prepared in a chloroform and formic acid mixture, leading to homogeneous solutions. The solution properties, including electrical conductivity, surface tension, and viscosity, were investigated with the EC, EC/TTE0.5, EC/TTE1.0, and EC/TTE1.5 solutions (Table 1) and are compiled in Table 2.
Adding TTE to the solutions reduced the electrical conductivity from 1.12 μS/cm (EC solution) to 0.63 μS/cm in the EC/TTE solution with 1.0 mL of TTE. Similarly, surface tension decreased from 32.6 mN/m in the EC solution to about 28 mN/m in the EC/TTE solutions with 0.5 and 1.0 mL of TTE and to 30.1 mN/m for the EC/TTE solution containing 1.5 mL of TTE (equivalent to 72.57% w/w of TTE relative to the mass of EC+TTE in the mixture). The viscosity of the EC solution (10% w/v), without TTE, was 9.8 mm2/s. In contrast, the EC/TTE solutions with 0.5 and 1.0 mL of TTE showed reduced viscosities of 8.3 and 8.2 mm2/s, respectively. The EC/TTE1.5 mixture exhibited a viscosity of 6.9 mm2/s.
These findings indicate that TTE oil significantly lowers the EC blends’ viscosity, surface tension, and electrical conductivity. Adjusting these parameters is crucial to optimize the electrospinning process—for example, Pavezi et al. [45] demonstrated that concentrations exceeding 10% v/v of acetic acid in chloroform/acetic acid binary mixtures can prevent the formation of microparticles during electrospraying of PLA solutions. By carefully controlling PLA concentration and solvent systems, they favored electrospinning over electrospraying. Additionally, Pavezi [45] emphasized that PLA (26 kDa) concentrations below 20% by mass do not result in fiber formation but particle formation via electrospraying.
The presence of TTE in the EC solution decreased its surface tension, likely due to TTE containing amphiphilic compounds similar to surfactants, which are known to reduce surface tension in solutions [46]. The EC/TTE1.5 solution exhibited a slight increase in surface tension (30.1 mN/m) compared to the EC/TTE0.5 and EC/TTE1.0 solutions. This increase can be attributed to the higher concentration of TTE (1.5 mL), which corresponds to 72.57% (w/w) relative to the EC concentration in the final mixture. The higher amount of TTE likely compensates for the surface tension reduction observed in lower TTE concentrations (about 28 mN/m in EC/TTE0.5 and EC/TTE1.0 solutions).
Viscosity measurements also reflected the influence of TTE concentration. The viscosity of the EC solution (without TTE) was 9.8 mm2/s. Adding 0.5 and 1.0 mL of TTE decreased the viscosity to 8.3 and 8.2 mm2/s, respectively. This reduction in viscosity can be attributed to the dilution effect caused by the addition of TTE, which lowers the overall concentration of EC in the solutions (Table 1). The EC/TTE1.5 mixture exhibited a greater viscosity reduction (6.9 mm2/s), further supporting this trend.
Volumes of 0.5, 1.0, or 1.5 mL of TTE were added to a 10% w/v EC solution prepared in 5 mL of chloroform/formic acid (85/15 v/v). This addition reduced the concentration of formic acid in the final mixture, thereby decreasing the electrical conductivity of the solutions. Formic acid is polar and has a high dielectric constant (58.5) [45]. The conductivity reduction observed in EC/TTE solutions is associated with the dilution of formic acid, which decreases its ability to accumulate charges for a given potential difference.
In summary, incorporating TTE into the EC solutions affects surface tension, viscosity, and electrical conductivity, with these properties varying depending on the concentration of TTE added to the polymer blend solution. These adjustments are critical for optimizing the electrospinning process of EC/TTE mixtures.

3.2. Fiber Characterization

EC solutions with and without TTE were electrospun under the experimental conditions in Table 1. The EC/TTE solutions were prepared using a binary solvent mixture of chloroform and formic acid at a ratio of 85/15 v/v, with varying volumes of TTE added. Previous studies have established that EC fibers can be successfully spun from solutions with concentrations ranging between 10% and 12% w/v, using solvent systems such as chloroform/formic acid and dichloromethane/formic acid [34].
SEM images of the fibers are presented in Figure 1. Fibers without TTE exhibited a significant presence of beads and a heterogeneous structure, with an average diameter of 478 ± 219 nm. The incorporation of TTE led to a notable reduction in fiber diameter due to decreased surface tension and viscosity of the solutions. This effect facilitated greater elongation of the polymer blend jet during electrospinning, resulting in thinner and more uniform fibers. Adding 0.5 mL of TTE leads to a 393 ± 120 nm diameter. Specifically, adding 1.0 mL of TTE imparted the smallest average diameter (252 ± 51 nm) compared to other conditions. When 1.5 mL of TTE was used, there was a slight increase in average fiber diameter (278 ± 59 nm) compared to the 1.0 mL TTE condition. This increase may be attributed to the higher surface tension observed in the EC/TTE1.5 solution compared to EC/TTE1.0. However, the difference in average fiber diameter between EC/TTE1.0 and EC/TTE1.5 was not statistically significant (Table 2).
Using 0.5 mL of TTE resulted in fibers with an average diameter of 293 ± 120 nm, corresponding to an EC/TTE ratio of 53/47 w/w in the EC/TTE0.5 solution. Meanwhile, the EC/TTE1.0 solution with a ratio of 36/64 w/w generated fibers with an average diameter of 252 ± 51 nm, and the EC/TTE1.5 solution with a ratio of 27/73 w/w resulted in fibers with an average diameter of 278 ± 59 nm (Figure 1). Overall, the presence of TTE reduced the average fiber diameter and minimized bead formation, with the most pronounced effect observed in the EC/TTE1.0 and EC/TTE1.5 mixtures (Figure 1).
An arithmetic mean of 150 random fiber diameter measurements was used for histogram representation in Figure 1. The EC/TTE mixtures presented optimal electrospinnability up to 1.5 mL of TTE added to the EC solution, beyond which there was a noticeable decrease in fiber homogeneity. The addition of TTE to the EC solutions resulted in a significant reduction in the average fiber diameter (p ≤ 0.95) (Table 2). Furthermore, TTE enhanced the homogeneity of the fibers, leading to narrower size distribution curves (Figure 1).
The water contact angle reflects a liquid’s adhesive and cohesive forces on a surface. Surfaces are categorized as super hydrophilic when their water contact angles are below 40°, hydrophilic between 40° and 90°, hydrophobic between 90° and 120°, and superhydrophobic when angles exceed 120° [47,48].
Table 2 presents the water contact angle results (degrees) for the fibers: 120° ± 2 for the EC sample, 97° ± 4 for EC/TTE0.5, 95° ± 5 for EC/TTE1.0, and 69° ± 1 for EC/TTE1.5. The EC, EC/TTE0.5, and EC/TTE1.0 fibers exhibit hydrophobic characteristics, while the EC/TTE1.5 sample, with a contact angle of 69° ± 1, is hydrophilic. This change can be attributed to the presence of terpinen-4-ol alcohol, a significant component of TTE. The main component of TTE (terpinen-4-ol) should increase the fiber’s polarity, facilitating interaction with water molecules through intermolecular hydrogen bonding [47,48].
The presence of TTE significantly enhances the hydrophilicity of the fibers, with the most notable effect observed at 1.5 mL of TTE (69° ± 1). This volume reduces the contact angle from 120° ± 2 (for fibers containing only EC) to 69° ± 1 (for fibers obtained with 1.5 mL of TTE in the EC/TTE mixture).
Vidal et al. [49] emphasize the significance of hydrophilic and hydrophobic components in biomedical applications, particularly wound treatment systems. They suggest that hydrophobic fibers, characterized by contact angles greater than 90°, are well-suited for wound dressings in treating skin wounds. The hydrophobic nature facilitates easy exchange and replacement of the material covering the wound. The EC, EC/TTE0.5, and EC/TTE1.0 fibers, with their low wettability and hydrophobic surfaces, meet the requirements for wound dressing applications when considering the wettability parameter alone.
Conversely, hydrophilic fibers, with contact angles less than 90°, are desirable for scaffolding applications where the material remains in contact with the tissue and aids in accelerating the healing process by promoting cell proliferation and tissue formation. In this context, the EC/TTE1.5 sample, exhibiting increased wettability, shows potential for application as a scaffold material. However, additional properties, such as surface roughness, mechanical strength, liquid absorption capacity (swelling behavior), biodegradability, stability, antimicrobial activity, and hemocompatibility, must be thoroughly investigated to determine the most suitable application for each material.
Figure 2 presents the DSC curves of EC and EC/TTE fibers. The EC DSC fiber profile displays an intense endothermic peak at 153 °C, which is more pronounced than the endothermic peaks observed in the DSC curves of the EC/TTE fibers. Additionally, increasing the TTE volume from 0.5 to 1.5 mL shifts the endothermic peak to lower temperatures than the endothermic peak temperature in the EC fiber DSC curve. The endothermic peak in the EC/TTE1.0 fiber DSC curve occurs at 153 °C, while in the EC/TTE1.5 sample, it shifts to 146 °C.
The presence of TTE is expected to alter the configuration of polymer chains in the blend, influencing interactions (mainly hydrophobic interactions) between polymer species in the EC blend. This effect modifies the profile of the endothermic peak in the DSC curves, altering the melting temperature of the EC blend in the presence of TTE. This change in the melting profile helps to explain the formation of thin fibers when TTE is present, as demonstrated in the SEM images.
Alves et al. [50] presented DSC curves of poly(3-hydroxybutyrate)/poly(ethylene glycol) films incorporated with rosemary essential oil. The presence of the crucial oil shifted the endothermic peaks related to the polymeric species to lower temperatures compared to the endothermic peak in the films obtained without the essential oil. Increasing the dosage of essential oil in the polymeric blend resulted in a reduction in the material’s final melting temperature. The results presented in this study align with those of Alves et al. [50], suggesting that the essential oil impacts the fibers’ surface and bulk properties. This alters the wettability and the profile of the DSC curves, respectively.
The FTIR-ATR spectra of TTE and the EC and EC/TTE1.5 fibers are presented in Figure 3. EC and EC/TTE1.5 were selected to evaluate the presence of TTE in the fiber. Intense and characteristic bands in the TTE FTIR spectrum at 1465, 1443, and 1378 cm−1 are attributed to stretching C-H bonds of methylene groups (–CH2) [51]. The band at 872 cm−1 is attributed to C-O-C stretching, which is present in the compound 1,8-cineole [51].
The FTIR spectra of the EC and EC/TTE1.5 fibers show bands at 1453 and 1455 cm−1, attributed to the stretching of the C=O bond (carboxylic acid and ester portions) found in Ecoflex® and PLA, respectively [34]. The bands at 1453 and 1455 cm−1 are also attributed to the asymmetric and symmetric stretching of C-H bonds in Ecoflex® and PLA [34]. The 1181 and 1182 cm−1 bands correspond to the symmetric and asymmetric stretching of C–O and C–O–C bonds (ester and carboxylic acid) found in Ecoflex® and PLA [35]. These bands confirm the presence of EC in the fibers. The band at 1181 cm−1 in the FTIR spectrum of the EC fiber shifts to 1182 cm−1. A similar effect occurs with the band at 1455 cm−1 in the FTIR spectrum of the EC fiber, which shifts to 1453 cm−1 and increases in intensity due to the presence of TTE in the fiber. This result indicates the presence of TTE in the EC fibers.
Figure 4 shows the high-resolution XPS spectra of the carbon envelopes (C1s) obtained on the surface of EC and EC/TTE1.5 fibers. The C1s envelopes exhibit peaks corresponding to aliphatic carbon atoms (C-C at approximately 286 eV), carbon atoms bonded to oxygen (C-O near 288 eV), and carbon atoms in carbonyl groups (C=O at approximately 290 eV). The chemical composition of TTE primarily includes hydrocarbons, terpenes, and alkyl alcohols [52]. Consequently, TTE is rich in aliphatic carbon. This composition explains the increase in the relative percentage of aliphatic carbon from 48.51% on the surface of EC fibers to 57.55% on the surface of EC/TTE1.5 fibers (Figure 4). The increase in aliphatic carbon content results in a corresponding decrease in the relative percentage of oxygen, which accounts for the reduction in C-O groups from 25.94% (EC fiber) to 22.94% (EC/TTE1.5 fiber) and the reduction in C=O groups from 25.55% (EC fiber) to 20.03% (EC/TTE1.5 fiber). These changes confirm the incorporation of TTE into the EC/TTE fibers.
Figure 5 displays the stress–strain curves of the electrospun fibers. The mechanical properties of the EC fibers (478 nm) included a tensile strength of 0.00254 MPa, elongation at break of 6.61%, and a Young’s modulus of 0.061 MPa. For the fibers containing TTE, the mechanical properties were as follows: EC/TTE0.5 (293 nm) had a tensile strength of 0.00654 MPa, an elongation at break of 3.70%, and a Young’s modulus of 0.240 MPa; EC/TTE1.0 (252 nm) had a tensile strength of 0.00497 MPa, an elongation at break of 4.91%, and a Young’s modulus of 0.111 MPa; and EC/TTE1.5 (278 nm) had a tensile strength of 0.00707 MPa, an elongation at break of 4.40%, and a Young’s modulus of 0.283 MPa.
The incorporation of TTE into the fibers significantly enhanced their mechanical properties. The presence of TTE increased both the tensile strength and Young’s modulus, indicating that TTE promotes the formation of stronger fibers with reduced plasticity. Specifically, TTE exhibited an anti-plasticizing effect, as evidenced by the substantial increase in Young’s modulus for EC/TTE0.5, EC/TTE1.0, and EC/TTE1.5 fibers compared to the EC fibers.
During the electrospinning of the EC blend, volatile compounds, such as solvents, evaporate. The electrospinning process also causes the evaporation of components from TTE, which is composed of low molecular weight volatile compounds. The boiling point of terpinen-4-ol is approximately 211 °C to 213 °C at standard atmospheric pressure [53]. Although the presence of TTE in the fibers was confirmed, part of the TTE should evaporate in the electrospinning process. Controlling the temperature and maintaining it at a level where the solvents evaporate but below the boiling points of the main TTE components would minimize the issue.

3.3. Antimicrobial Activity of the Tea Tree Essential Oil

High concentrations (about 7.5 mg/mL) of TTE are required to inhibit and achieve bactericidal activity. Other studies have indicated MIC and MBC in the range of 17 to 35 mg/mL against 30 different isolates of S. aureus [54]. These MIC and MBC results were estimated from percentage volume/volume concentrations, considering a density of 0.8819 g/mL for TTE. No MIC and MBC data for P. aeruginosa have been reported in the literature. However, the major component of TTE, terpinen-4-ol, has shown MIC and MBC in the range of 8% v/v against P. aeruginosa [55]. When this value is converted to mg/mL using the density of 0.8819 g/mL for TTE, the MIC and MBC values are approximately 70 mg/mL. The results obtained in this study differ slightly from those reported in the literature, especially concerning S. aureus. These differences are likely due to the variable composition of TTE.
Figure 6 shows digital images of Petri dishes containing agar seeded with microbial suspensions after MIC determination. The upper panel illustrates the effect of TTE concentration on S. aureus. In the S. aureus test, microbial growth inhibition at concentrations of 7.5 mg/mL and 15 mg/mL reached percentages higher than 99.999%. This result is based on the initial concentration of S. aureus (500 μL at 107 CFU) seeded with fibers in the MIC determination microdilution test. At a concentration of 3.75 mg/mL, there was no inhibition of S. aureus. Increasing the dosage to 7.5 mg/mL reduced colony-forming units (CFU) to 12. At a 15 mg/mL concentration, the number of colonies reduced to just three, indicating inhibition higher than 99.9999%.
The lower panel presents the results against P. aeruginosa (Figure 6). A concentration of 3.75 mg/mL of TTE did not inhibit microbial growth; however, concentrations of 7.5 mg/mL and 15 mg/mL significantly reduced the CFU to 20 and 19 (about 99.999% of inhibition), respectively. These results confirm the antimicrobial activity of TTE against both Gram-positive bacteria (S. aureus) and Gram-negative bacteria (P. aeruginosa).

3.4. Antiadhesive and Antimicrobial Activity of the Fibers

SEM images of polystyrene control and fibers after 24 h of contact with S. aureus and P. aeruginosa are presented in Figure 7. Generally, bacteria adhered more to the surface of the polystyrene control and EC fibers. More S. aureus cells are observed on the fibers than P. aeruginosa cells. The S. aureus adhered to the surface of the polystyrene control, and fibers exhibited regular morphology (cocci, spheres), indicating that the samples do not have cytotoxic effects on Gram-positive S. aureus cells [56,57].
In contrast, P. aeruginosa cells did not completely cover the surfaces of EC/TTE0.5, EC/TTE1.0, and EC/TTE1.5 fibers as they did with the polystyrene control and EC fibers. This suggests that the fiber surface exhibits antiadhesive potential against P. aeruginosa, confirmed by control tests with the EC fiber and polystyrene film. P. aeruginosa appears to adhere more to the surface of TTE-free fibers than to fibers containing TTE. As expected, adhesion is also more pronounced on the polystyrene surface since this material lacks antiadhesive and antimicrobial activity [12].
EC/TTE0.5, EC/TTE1.0, and EC/TTE1.5 fibers seem to demonstrate biocidal activity against P. aeruginosa. Some microbial cells adhered to the surface of TTE-containing fibers do not exhibit the regular rod-shaped morphology (bacilli) seen on the surface of polystyrene. The presence of irregularities and greater heterogeneity in EC fibers complicates the comparison of microbial adhesion and proliferation results with TTE-containing fibers. However, P. aeruginosa cells with regular morphology are also observed on the surface of EC fibers. Additionally, regions where P. aeruginosa cells are aggregated on the surface of EC/TTE0.5, EC/TTE1.0, and EC/TTE1.5 fibers are visible, particularly in EC/TTE1.5 fiber.
The disk diffusion assay did not indicate the formation of inhibition zones against S. aureus and P. aeruginosa. It is suggested that the TTE interacts with the fibers through attractive van der Waals forces, as mechanical tests indicated an anti-plasticizing effect. These interactions (dipole–dipole and London dispersion) likely inhibit the release of TTE onto the agar-seeded Petri dish, thereby preventing the formation of inhibition zones.

3.5. Blood Coagulation

When any injury exposes blood, the body initiates the coagulation process, involving physical and chemical changes in the blood through various factors. Platelet adhesion on fiber surfaces indicates thrombogenicity, which can lead to platelet activation and the start of the coagulation cascade [49]. During this process, blood loses its fluid properties and solidifies due to coagulation. Wound dressings should facilitate blood coagulation in damaged skin tissues to prevent bleeding.
Figure 8 shows fluorescence images of fibers and a control (glass surface) in contact with human blood platelets, stained with calcein-AM dye after 2 h of incubation. Calcein-AM highlights the platelets adhered to the fiber surface, appearing as green staining. Platelet adhesion on the fiber surface indicates that blood coagulation will likely occur on the fiber surface, suggesting low hemocompatibility [49].
Fluorescence images reveal that platelets preferentially adhere to the surface of EC/TTE0.5 fiber, even compared to the control assay conducted with glass, which is known to be non-hemocompatible. This result implies that the surface of EC/TTE0.5 fiber is prone to blood coagulation, indicating low blood compatibility. Overall, platelets adhered to all fiber surfaces, as confirmed by the fluorescence images (Figure 8).
The percentage of surface area covered by platelets is presented in Figure 9. The area covered by platelets on the surface of EC/TTE0.5 fiber was 17.5%, which is significantly higher than the coverage on other samples, none of which exceeded 0.20% (p ≤ 0.05). This result suggests that EC/TTE0.5 fiber may be suitable for covering damaged skin tissues exposed to bleeding. In such cases, the fiber could act as a wound dressing, promoting blood coagulation on the skin and preventing blood loss at the injury site.
The fluorescence images indicate platelet deposition on the surface of all samples, though it is less pronounced in the EC and EC/TTE1.5 samples. This suggests a low compatibility between human blood and the fibers. Figure 9b confirms these findings through UV–vis absorbance measurements taken after bringing the fibers and a glass control sample into contact with human blood for 15 min.
Blood coagulation is a complex process that significantly affects the optical properties of blood samples. As coagulation progresses, it reduces the concentration of suspended red blood cells (erythrocytes) in the liquid portion of the blood. This decrease in suspended erythrocytes directly impacts the sample’s light absorption characteristics, particularly at a wavelength of 540 nm [58]. The reduction in absorbance indicates blood coagulation when in contact with the surface of the fibers and the glass (control sample). After 15 min of allowing coagulation to occur, water is added to the sample. This addition causes hemolysis (rupture) of the erythrocytes that are not part of the coagulated blood. Hemolysis releases hemoglobin from these non-coagulated cells into the solution. The amount of released hemoglobin is then quantified through absorbance measurements at 540 nm, providing an inverse measure of the degree of coagulation that occurred during the initial 15 min period (Figure 9b). A lower absorbance at this stage indicates more extensive initial coagulation, as fewer erythrocytes undergo hemolysis.
At t = 0, the absorbance of human blood was around 2.195. After 15 min, the absorbance values dropped to 0.531 for the blood in contact with EC, 0.309 for EC/TTE0.5, and 0.668 for EC/TTE1.5 (Figure 9b). These results indicate that all surfaces induce coagulation, but the EC/TTE0.5 fiber exhibits a significant effect. Notably, the EC/TTE0.5 sample was the only one that showed statistically different coagulation results compared to the glass control sample (p ≤ 0.05), which supported an absorbance of 0.901 after 15 min of contact (Figure 9b).

4. Conclusions

This study reported the production of Ecovio® (EC) fibers using the electrospinning technique. Challenges arose due to EC’s hydrophobic nature and solubility in low-polarity solvents. To address this, tea tree essential oil (TTE) was added to EC solutions in varying volumes of 0, 0.5, 1.0, and 1.5 mL. The addition of TTE improved the homogeneity of the fibers and enabled the production of thin, sphere-free fibers with an average diameter of 252 ± 51 nm. Furthermore, TTE altered the fibers’ wettability, with 1.5 mL of TTE producing hydrophilic fibers. TTE also enhanced the mechanical properties, increasing the fibers’ modulus of elasticity from 0.00254 MPa (pure EC fiber) to 0.00707 MPa.
The antimicrobial results demonstrated that TTE provided significant activity against S. aureus and P. aeruginosa at 7.5 mg/mL, inhibiting at least 99.99% of bacteria in suspension. EC/TTE fibers exhibited antiadhesive and cytotoxic properties against P. aeruginosa, with reduced bacterial growth on the fiber surfaces. However, EC/TTE fibers, particularly those with 0.5 mL of TTE, showed low hemocompatibility compared to glass. In conclusion, EC/TTE fibers possess several properties desirable for biomedical wound dressings, including inhibition of bacterial adhesion and growth and the ability to coagulate human blood. Therefore, EC/TTE0.5 and EC/TTE1.5 fibers may have potential applications in treating skin wounds.

Author Contributions

Conceptualization, B.Z.d.S., D.P.F., and A.F.M.; methodology, B.Z.d.S., D.P.F., and S.P.F.; software, B.Z.d.S. and A.F.M.; validation, B.Z.d.S. and E.G.B.; formal analysis, C.F.T., D.A.d.A., and A.F.M.; investigation, B.Z.d.S., D.P.F., S.P.F., and D.A.d.A.; resources, M.J.K., K.C.P., and A.F.M.; writing—original draft preparation, B.Z.d.S. and C.F.T.; writing—review and editing, E.G.B., M.J.K., K.C.P., and A.F.M.; visualization, A.F.M.; supervision, A.F.M. and E.G.B.; project administration, A.F.M., and E.G.B. All authors have read and agreed to the published version of the manuscript.

Funding

This research was funded by the “National Council for Scientific and Technological Development—CNPq” for financial support (grant 305579/2023-1). This study was financed in part by the Coordenação de Aperfeiçoamento de Pessoal de Nível Superior—Brasil (CAPES)-Finance Code 001.

Data Availability Statement

The data presented in this study are available on request from the corresponding author due to privacy or ethical restrictions.

Acknowledgments

The authors thank the State University of Maringá (Complex Research Center—COMCAP) and Federal University of Technology (the multiuser laboratories at Apucarana and Londrina) for the performed analysis.

Conflicts of Interest

The authors declare no conflicts of interest.

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Figure 1. SEM images of the EC and EC/TTE fibers obtained from the solutions listed in Table 1. Labels: EC = the Ecovio® polymer blend composed of 55% poly(butylene adipate-co-terephthalate) (PBAT) and 45% poly(lactic acid) (PLA); TEE: tea tree essential oil with a density of 0.8818 g/mL; EC/TTE0.5, EC/TTE1.0, and EC/TTE1.5 are the electrospun solutions which resulted in fibers after electrospinning, prepared by adding 0.5 mL, or 1.0 mL, or 1.5 mL of TTE into an EC solution at 10% w/v, respectively.
Figure 1. SEM images of the EC and EC/TTE fibers obtained from the solutions listed in Table 1. Labels: EC = the Ecovio® polymer blend composed of 55% poly(butylene adipate-co-terephthalate) (PBAT) and 45% poly(lactic acid) (PLA); TEE: tea tree essential oil with a density of 0.8818 g/mL; EC/TTE0.5, EC/TTE1.0, and EC/TTE1.5 are the electrospun solutions which resulted in fibers after electrospinning, prepared by adding 0.5 mL, or 1.0 mL, or 1.5 mL of TTE into an EC solution at 10% w/v, respectively.
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Figure 2. DSC curves of the EC and EC/ETT fibers. Labels: EC = the Ecovio® polymer blend composed of 55% poly(butylene adipate-co-terephthalate) (PBAT) and 45% poly(lactic acid) (PLA); TEE: tea tree essential oil with a density of 0.8818 g/mL; EC/TTE0.5, EC/TTE1.0, and EC/TTE1.5 are the electrospun solutions which resulted in fibers after electrospinning, prepared by adding 0.5 mL, or 1.0 mL, or 1.5 mL of TTE into an EC solution at 10% w/v, respectively.
Figure 2. DSC curves of the EC and EC/ETT fibers. Labels: EC = the Ecovio® polymer blend composed of 55% poly(butylene adipate-co-terephthalate) (PBAT) and 45% poly(lactic acid) (PLA); TEE: tea tree essential oil with a density of 0.8818 g/mL; EC/TTE0.5, EC/TTE1.0, and EC/TTE1.5 are the electrospun solutions which resulted in fibers after electrospinning, prepared by adding 0.5 mL, or 1.0 mL, or 1.5 mL of TTE into an EC solution at 10% w/v, respectively.
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Figure 3. FTIR-ATR spectra of TTE, EC fiber, and EC/TTE1.5 fiber.
Figure 3. FTIR-ATR spectra of TTE, EC fiber, and EC/TTE1.5 fiber.
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Figure 4. High-resolution XPS spectra for C1 peaks obtained from EC and EC/TTE1.5 fibers.
Figure 4. High-resolution XPS spectra for C1 peaks obtained from EC and EC/TTE1.5 fibers.
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Figure 5. The stress–strain curves of the fibers.
Figure 5. The stress–strain curves of the fibers.
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Figure 6. Digital images of Petri dishes containing agar seeded with 10 μL of microbial suspension of S. aureus and P. aeruginosa.
Figure 6. Digital images of Petri dishes containing agar seeded with 10 μL of microbial suspension of S. aureus and P. aeruginosa.
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Figure 7. SEM images of polystyrene control (PS) and EC/TTE fibers seeded with S. aureus and P. aeruginosa after 24 h of contact.
Figure 7. SEM images of polystyrene control (PS) and EC/TTE fibers seeded with S. aureus and P. aeruginosa after 24 h of contact.
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Figure 8. Fluorescence images of fibers and control test (glass) after contact with human blood platelets for 2 h of incubation. The platelets were stained with calcein-AM, emitting a green coloration in the fluorescence images.
Figure 8. Fluorescence images of fibers and control test (glass) after contact with human blood platelets for 2 h of incubation. The platelets were stained with calcein-AM, emitting a green coloration in the fluorescence images.
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Figure 9. (a) Percentages of surface area covered by platelets obtained through analysis of fluorescence images using ImageJ software. The ****, ***, and * indicates significant results with p ≤ 0.001, p ≤ 0.01, and p ≤ 0.05, respectively. (b) Blood coagulation results from human blood exposure to the fibers and control (glass). The term “blood (t = 0)” in Figure “b” refers to the absorbance of hemolyzed erythrocytes obtained from fresh human blood at time zero, meaning before any contact with the fibers and glass.
Figure 9. (a) Percentages of surface area covered by platelets obtained through analysis of fluorescence images using ImageJ software. The ****, ***, and * indicates significant results with p ≤ 0.001, p ≤ 0.01, and p ≤ 0.05, respectively. (b) Blood coagulation results from human blood exposure to the fibers and control (glass). The term “blood (t = 0)” in Figure “b” refers to the absorbance of hemolyzed erythrocytes obtained from fresh human blood at time zero, meaning before any contact with the fibers and glass.
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Table 1. Chemical solutions used in the electrospinning.
Table 1. Chemical solutions used in the electrospinning.
SolutionsEC (% w/v)TTE (mL)TTE (% w/v)EC/TTE (% w/w)
EC1000100/0
EC/TTE0.59.10.58.8253.1/46.9
EC/TTE1.08.31.017.636.2/63.8
EC/TTE1.57.71.526.427.4/72.6
EC: Ecovio® polymer blend; TTE: tea tree essential oil. The w/v and w/w indicate the weight/volume and weight/weight ratios; concentrations are in percentages.
Table 2. The solution properties (electrical conductivity, surface tension, and viscosity), the average size of the electrospun fibers, and the water contact angles (WCAs) measured on the fibers.
Table 2. The solution properties (electrical conductivity, surface tension, and viscosity), the average size of the electrospun fibers, and the water contact angles (WCAs) measured on the fibers.
SolutionsConductivity (μS/cm)Surface Tension (mN/m)Viscosity (mm2/s)Size (nm) 1WCA (°) 1
EC1.12 ± 0.12 a32.6 ± 0.4 a9.8 ± 0.2 a478 ± 219 a120 ± 2 a
EC/TTE0.51.07 ± 0.10 a28.1 ± 0.2 b8.3 ± 0.1 b393 ± 120 b97 ± 4 b
EC/TTE1.00.63 ± 0.08 b28.2 ± 0.2 b8.2 ± 0.2 b252 ± 51 b95 ± 5 b
EC/TTE1.50.74 ± 0.07 b30.1 ± 0.2 c6.9 ± 0.1 c278 ± 59 b69 ± 1 c
1 Results for average fiber size and water contact angles (WCAs) were obtained from the electrospun fibers produced using the solutions listed in Table 1. Different superscript letters indicate statistically significant differences within each column (p ≤ 0.95).
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MDPI and ACS Style

de Souza, B.Z.; Facchi, D.P.; Facchi, S.P.; Teodoro, C.F.; de Almeida, D.A.; Popat, K.C.; Kipper, M.J.; Bonafé, E.G.; Martins, A.F. Electrospun Fibers of Ecovio® Polymer Blends with Antimicrobial Tea Tree Essential Oil: Enhanced Chemical and Biological Properties. Processes 2024, 12, 2330. https://doi.org/10.3390/pr12112330

AMA Style

de Souza BZ, Facchi DP, Facchi SP, Teodoro CF, de Almeida DA, Popat KC, Kipper MJ, Bonafé EG, Martins AF. Electrospun Fibers of Ecovio® Polymer Blends with Antimicrobial Tea Tree Essential Oil: Enhanced Chemical and Biological Properties. Processes. 2024; 12(11):2330. https://doi.org/10.3390/pr12112330

Chicago/Turabian Style

de Souza, Bianca Z., Débora P. Facchi, Suelen P. Facchi, Carlos F. Teodoro, Débora A. de Almeida, Ketul C. Popat, Matt J. Kipper, Elton G. Bonafé, and Alessandro F. Martins. 2024. "Electrospun Fibers of Ecovio® Polymer Blends with Antimicrobial Tea Tree Essential Oil: Enhanced Chemical and Biological Properties" Processes 12, no. 11: 2330. https://doi.org/10.3390/pr12112330

APA Style

de Souza, B. Z., Facchi, D. P., Facchi, S. P., Teodoro, C. F., de Almeida, D. A., Popat, K. C., Kipper, M. J., Bonafé, E. G., & Martins, A. F. (2024). Electrospun Fibers of Ecovio® Polymer Blends with Antimicrobial Tea Tree Essential Oil: Enhanced Chemical and Biological Properties. Processes, 12(11), 2330. https://doi.org/10.3390/pr12112330

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