Antimicrobial Characterization of Advanced Materials for Bioengineering Applications

Summary

We present a protocol for the antimicrobial characterization of advanced materials. Here, the antimicrobial activity on material surfaces is measured by two methods that complement each other: one is based on the agar disk diffusion test, and the other is a standard procedure based on the ISO 22196:2007 norm.

Abstract

The development of new advanced materials with enhanced properties is becoming more and more important in a wide range of bioengineering applications. Thus, many novel biomaterials are being designed to mimic specific environments required for biomedical applications such as tissue engineering and controlled drug delivery. The development of materials with improved properties for the immobilization of cells or enzymes is also a current research topic in bioprocess engineering. However, one of the most desirable properties of a material in these applications is the antimicrobial capacity to avoid any undesirable infections. For this, we present easy-to-follow protocols for the antimicrobial characterization of materials based on (i) the agar disk diffusion test (diffusion method) and (ii) the ISO 22196:2007 norm to measure the antimicrobial activity on material surfaces (contact method). This protocol must be performed using Gram-positive and Gram-negative bacteria and yeast to cover a broad range of microorganisms. As an example, 4 materials with different chemical natures are tested following this protocol against Staphylococcus aureus, Escherichia coli, and Candida albicans.The results of these tests exhibit non-antimicrobial activity for the first material and increasing antibacterial activity against Gram-positive and Gram-negative bacteria for the other 3 materials. However, none of the 4 materials are able to inhibit the growth of Candida albicans.

Introduction

Implant failure is often a consequence of microbial infections that occur in spite of antimicrobial prophylaxis and aseptic working conditions. This problem is causing very high healthcare costs and is distressing among patients¹. Important bacteria such as Staphylococcus aureus are currently considered to be very dangerous pathogens in nosocomial infections associated with catheters and other medical implants and are the main contaminants of medical instruments². Therefore, the development of novel antimicrobial strategies is urgently needed for both daily and medical uses.

Antimicrobial agents include antibiotics³, quaternary ammonium compounds⁴, metal ions/oxides⁵, and antimicrobial peptides (AMPs)⁶. Antibiotics are gradually becoming less efficient due to bacterial resistance⁷, which is on the rise due to antibiotic overuse⁸. Quaternary ammonium compounds are only very efficient for a short-term use because of microbial resistance⁹. Metal ions/oxides have long been utilized as very effective antimicrobial agents and are used in many common commercial products including bandages, water filters, paints, etc.^10,11,12. However, it has been demonstrated that these types of compounds can be toxic to some types of mammalian cells¹³.

AMPs show excellent antimicrobial and immunomodulatory properties^14,15, and bacteria seem to find it very difficult to develop a resistance against them¹⁶. However, the process to produce pure AMPs is expensive; therefore, a large-scale production is not viable. Thus, strategies to counter the problems in producing AMPs have been developed (e.g., small molecular antibacterial peptoid mimics¹⁷, peptoids¹⁸, α-peptides¹⁹ and β-peptides²⁰). Methacrylate-ended polypeptides and polypeptoids have been synthesized for antimicrobial and antifouling coatings²¹.

The development of new antimicrobial agents such as advanced materials in pure or hybrid form, able to prevent and treat multidrug-resistant infections, is increasingly necessary. A broad range of new advanced materials for many bioengineering fields such as tissue and bioprocess engineering have been developed with improved chemical and physical properties in the last decades through several methods: plasma-polymerization grafting onto a hydrophobic substrate^22,23,24, tailoring of crosslinking density^25,26, polymerization in solution^27,28,29,30, porogen dissolution^31,32, and by the incorporation of nanomaterials such as graphene oxide (GO)^33,34,35,36 and carbon nanofibers (CNFs)³⁷.

The study of the antimicrobial capacity of these new materials could exponentially increase their potential bioengineering applicability and has, therefore, become essential. We present an easy-to-follow protocol to quantify the antimicrobial activity of such new advanced materials. Here, after the sample preparation, two complementary methods are followed: the first is based on the agar disk diffusion test³⁸ (diffusion method) and the second is based on the ISO 22196:2007 norm³⁹ to measure the antimicrobial activity on material surfaces (contact method).

Protocol

1. Sample Preparation

1. Cut the material samples into 10 mm diameter disks with a 10 mm diameter cylindrical punch.
   NOTE: Brittle materials can be softened in suitable sterile solvents for 1 h and then cut into disks. For example, hydrophilic materials such as zinc alginate were tested following this protocol and were moistened in autoclaved water before cutting them in order to avoid sample breaking. However, other hydrophobic materials such as poly(3-hydroxybutyrate-co-3-hydroxyvalerate) do not need any kind of previous swelling in order to be properly cut.
2. Dry the sample material disks at 60 °C in a vacuum oven (<10^-2 Torr) for 24 h.
   NOTE: Some materials may need a high drying temperature. However, it is important not to reach a temperature that could thermally degrade the material.
3. Measure the material film thicknesses with a digital caliper.
   NOTE: This protocol recommends the utilization of material films with constant and similar thicknesses when comparing the antimicrobial activity of different materials.
4. Sterilize each specimen by immersion in ethanol 70% for 10 min and subsequent ultraviolet (UV) radiation for 1 h per each side.
   NOTE: UV radiation can be performed placing each specimen in a sterile Petri dish inside a laminar flow hood with a 12.0 W lamp of UV-C radiation.
   CAUTION: Researchers should not expose themselves to UV radiation, because it is mutagenic.
5. Perform steps 1.1, 1.2, 1.3 and 1.4. with the control material disks. 
   NOTE: Polyethylene terephthalate (PET) or alternative non-antimicrobial materials could be used as control disks in the diffusion and contact method. Furthermore, when characterizing nanocomposites or treated materials, the base material should be used as control material.

2. Recommended Microorganisms

NOTE: We recommend the use of 3 different microorganisms to study the antimicrobial capacity of the tested material against a wide range of microorganisms.

1. Use pure cultures of 3 microorganisms: the Gram-positive bacteria Staphylococcus aureus, the Gram-negative bacteria Escherichia coli, and the yeast Candida albicans.
   NOTE: Other microorganism species can also be tested with this protocol by modifying the incubation conditions if necessary.
   CAUTION: The required biosafety measurements must be followed according to the type of microorganism employed in this protocol.
2. Work with pre-sterile or autoclaved material and use a Bunsen burner during the whole process of the microbial manipulation or a biological safety cabinet (if necessary) to ensure aseptic conditions.
   NOTE: Recommended autoclave conditions are 121 °C during 15 min for culture mediums and 121 °C during 20 min for the working material and biological residues.

3. Agar Disk Diffusion Test (Diffusion Method)

NOTE: When a liquid diffusion of antimicrobial compounds might be the main antimicrobial mechanism of advanced materials, the diffusion method can provide very useful information about the antimicrobial capacity of these materials. The material disk located at the center of the agar plate can form a transparent ring zone (halo) where a growth inhibition of microorganisms occurs after 24 h of culture (see Figure 1).

1. Diffusion test procedure
   1. Prepare and autoclave tryptic soy agar (TSA) following the manufacturer’s instructions.
   2. Pour the TSA into sterile Petri dishes under aseptic conditions using a Bunsen burner or a laminar flow hood.
      NOTE: The TSA plates must be 4–6 mm thick.
   3. Culture the different microorganisms to be tested aerobically for 18–24 h in the Petri dishes with TSA in an incubator at 37 °C.
   4. Prepare and autoclave tryptic soy broth (TSB) following the manufacturer’s instructions.
   5. Pour the TSB in a 50 mL pre-sterilized centrifuge tube with a pre-sterilized serological pipette under aseptic conditions using a Bunsen burner or a laminar flow hood.
   6. Resuspend a few colonies from step 3.1.3 in 25 mL of TSB contained in a sterile centrifuge tube using a sterile cotton swab and vortex them for 1 min to achieve a uniform mixing.
   7. Adjust the absorbance (at 540 nm) of the culture with a spectrophotometer to the suitable number of colony forming units (CFU) per mL: approximately 1.5 x 10⁸ CFU/mL for bacteria and from 1 x 10⁶ to 5 x 10⁶ CFU/mL for yeast.
      NOTE: The culture and cuvette volumes to measure the absorbance must be selected according to the type of spectrophotometer utilized.
   8. Vortex the microbial broth for 5 seconds to improve the microorganism dispersion and briefly submerge a sterile cotton swab in this microbial suspension. Remove the excess of liquid from the swab by pressing it against the tube wall containing the culture.
   9. Evenly streak the microbial broth suspension with the sterile cotton swab onto the surface of the TSA plates in 3 planes to cover their whole surface with the microorganism and let it dry for 5 min after the inoculation.
      NOTE: To remove any moisture, the TSA plates must be placed open in an inverted position at 37 °C for 10–15 min before the inoculation.
   10. Sterilize a pair of tweezers by immersing them in a beaker with ethanol 96% and then flaming them with a Bunsen burner or alcohol burner.
   11. Place the sample disks to be tested and control disk at the center of the TSA plates using the pair of sterile tweezers.
   12. Incubate aerobically the TSA plates in an inverted position at 37 °C for 24 h.
       NOTE: In order to avoid any contamination risk, it is recommended to incubate the TSA plates in an inverted position. However, if the sample disk detaches from the TSA plates, do not perform this step in an inverted position. In this case, it is recommended to dry the plates in the laminar flow hood. This antimicrobial test must be performed at least in quadriplicate on different days to ensure reproducibility.
2. Checking of microbial suspension concentration and purity
   NOTE: The following steps are necessary in order to check that the microbial concentration determined with the spectrophotometer in step 3.1.7 is correct and ensure that there was no microbial environmental contamination. A microbial environmental contamination can be easily detected by the appearance of various types of microbial colonies after 24 h of culture. Furthermore, no microbial contamination of the TSB medium during its manipulation in the decimal serial dilutions must be ensured with a negative TSB control plate.
   1. Dispense the sterile TSB (prepared in step 3.1.4) into sterile microcentrifuge tubes using a micropipette with suitable autoclaved tips in aseptic conditions. One of them will be utilized as a negative TSB control.
   2. Perform decimal serial dilutions with the microbial broth suspension utilized in step 3.1.9 in the sterile microcentrifuge tubes containing TSB.
   3. Spread 100 µL of each dilution on TSA plates using a pre-sterilized Drigalski spatula or an alternative instrument. Also spread 100 μL of TSB medium without microorganism (prepared in step 3.2.1) on a TSA plate as a negative TSB control plate.
   4. Incubate aerobically the TSA plates aerobically at 37 °C for 24 h.
   5. Count the number of colonies to check that the CFU/mL are similar to that determined in step 3.1.7.
   6. Check that there is no microbial environmental contamination on the TSA plates with only one type of colonies.
   7. Check that there is no microbial contamination on the TSB negative control plate showing no colonies

4. Measurement of Antimicrobial Activity on Material Surfaces (Contact Method)

NOTE: When surface contact might be the main antimicrobial mechanism of some advanced materials, the contact method can provide very useful information about the antimicrobial capacity of these materials. In this method, the microorganisms are placed directly onto the material surface and their growth inhibition can be determined after a certain amount of time.

1. Initial procedure
   1. Prepare and autoclave TSB following the manufacturer’s instructions.
   2. Pour the TSB in a 50 mL pre-sterilized centrifuge tube with a pre-sterilized serological pipette under aseptic conditions using a Bunsen burner or a laminar flow hood.
   3. Culture the different microorganisms to be tested aerobically overnight in the tube with TSB in an orbital shaker (140 rpm) at 37 °C.
   4. Dilute the overnight culture in 20 mL of TSB in a 50 mL pre-sterilized centrifuge tube to a concentration of approximately 10⁶ CFU/mL (determined with a spectrophotometer at 540 nm).
      NOTE: The culture and cuvette volumes to measure the absorbance must be selected according to the type of spectrophotometer utilized.
   5. Perform decimal serial dilutions of this culture in sterile microcentrifuge tubes containing TSB. Spread 100 µL of the culture on TSA plates and incubate it aerobically at 37 °C for 24 h. 
   6. Count the number of colonies to ensure an initial cell concentration of approximately 1 x 10⁶ CFU/mL
   7. Place 4 control disks for microbial counting after 24 h and 4 sample disks of each type of the tested materials for microbial counting after 24 h in separates wells of a sterile 48-well plate.
   8. Pipette 150 µL of the microbial suspension onto each disk surface.
2. Microbial counting on the control and tested materials (after 24 h)
   1. After step 4.1.6, aerobically incubate the 4 sample disks remaining in the 48-well plate at 37 °C for 24 h.
      NOTE: This 24 h incubation time can be modified in order to study the growth inhibition at shorter or longer times.
   2. After 24 h of incubation, pipette 850 µL of sterile PBS onto the surface of the 4 sample disks and mix it with the 150 µL of the microbial suspension.
   3. Collect the PBS/microbial suspension mixture and each disk from the 48-well plate and transfer them to a 10 mL pre-sterilized tube.
   4. Vortex the PBS/microbial suspension mixture and each disk for 1 min, sonicate it at 50 Hz for 5 min and vortex it again for 1 min to ensure that no viable microorganisms remain adhered to the material surface.
   5. Perform decimal serial dilutions of each sonicated culture in sterile microcentrifuge tubes containing TSB and spread 100 µL of the culture on TSA plates and incubate it aerobically at 37 °C for 24 h.
   6. Count the number of colonies, which are the number of viable microorganisms on each sample and control disk surface. Express this number of viable cells in (CFU/mL).
   7. Take a photograph of the final microbial culture for the sample and control disks.

5. Antimicrobial Results Analysis

Figure 1: Measurements for the normalized width of the antimicrobial "halo". This panel shows the diameter of the inhibition zone (d_iz) and the disk diameter (d). Please click here to view a larger version of this figure.

1. Diffusion method results analysis
   1. Measure the diameter of the inhibition zone (d_iz) and the disk diameter (d) (see Figure 1) with a digital caliper.
      NOTE: The inhibition zone or antimicrobial “halo” is formed as a consequence of the microbial growth inhibition produced by the antimicrobial material disk (see Figure 1). It is possible to observe that there is a transparent ring zone close to the sample in comparison with the rest of the plate where the microorganisms have grown properly (opaque zone).
   2. Determine the normalized width of the antimicrobial “halo” (nw_halo) of each disk by applying equation (1).
      (1)     
   3. Determine the mean and standard deviation of the normalized width of the antimicrobial “halo” with the 4 determined nw_halo values of each sample.
   4. Take a photograph of the final microbial culture with the material disk.
      Note: The diameter of the inhibition zone (d_iz) and the disk diameter (d) can also be measured from the photograph taken in step 5.1.4 by using a suitable image processing software.
2. Contact method results analysis
   1. Determine the number of viable microorganisms recovered according to equation (2).
      (2)     
      NOTE: Here, N is the number of viable microorganisms recovered per cm² per test specimen; C is the plate count; D is the dilution factor; A is the surface area of the test specimen in cm² determined with the sample disk diameter.
   2. Determine the loss of viability (LV) to reflect the inhibition of cell growth by applying equation (3).
      (3)     
      NOTE: Here, C is the average number of viable microorganisms (N) in CFU/mL•cm², recovered from the control specimens after 24 h; S is the number of viable microorganisms (N) in CFU/mL•cm², recovered from the test specimens after 24 h.
   3. Determine the mean and standard deviation of the loss of viability with the 4 determined LV(%) values of each sample.

Results

This protocol was employed, as an example, to test the antimicrobial capacity of 4 materials with different chemical natures against the 3 recommended microorganisms: Staphylococcus aureus, Escherichia coli, and Candida albicans.The results of the agar disk diffusion tests (diffusion method) exhibited non-antimicrobial activity for the first material (M1) as it occured in the control disk (C, image not shown) and increasing antibacterial activity against Gram-positive and Gram-negative bacteria for the other 3 materials M2, M3 and M4 (see Figure 2).

Figure 2: Antimicrobial diffusion method results. This panel shows the antimicrobial diffusion method for the 4 material (M1, M2, M3, and M4) disks (10 mm diameter x 1 mm thickness) against S. aureus and E. coli after 24 h of incubation. Please click here to view a larger version of this figure.

Figure 3 shows the different normalized widths of the antimicrobial "halo" (nw_halo) for the different example materials M1, M2, M3, and M4 against Gram-positive and Gram-negative bacteria calculated with equation (1). However, none of the 4 materials were able to inhibit the growth of the yeast Candida albicans (images not shown).

Figure 3: Antimicrobial diffusion "halo" results. This panel shows the normalized "halo" (nw_halo) for each material (M1, M2, M3, and M4) disk (10 mm diameter x 1 mm thickness) against S. aureus and E. coli after 24 h of incubation. The differences are statistically significant (p <0.01). However, sample M1 exhibited no antimicrobial activity. Please click here to view a larger version of this figure.

The results of the contact method also exhibited non-antimicrobial activity for the first material (M1) as it occurred in the control disk (C) and increasing antibacterial activity against Grampositive and Gram-negative bacteria for the other 3 materials (see Figure 4).

Figure 4: Antimicrobial contact method results. This panel shows the respective 90 mm plates of the 4 material (M1, M2, M3, and M4) surface antimicrobial activity assay according to the ISO 22196:2007 after 24 h of incubation for S. aureus and E. coli (dilution factor of 10^-4). C is the viable bacteria recovered from the control disk after 24 h of incubation. Please click here to view a larger version of this figure.

The loss of viability (%) was determined by equation (2) and (3) as indicated in this protocol (see Figure 5).

Figure 5: Loss of viability by contact method. This panel shows the loss of viability (%) for M1, M2, M3, and M4 against S. aureus and E. coli on the material surfaces. Sample M1 exhibited no antimicrobial activity. Please click here to view a larger version of this figure.

However, none of the 4 materials were able to inhibit the growth of the yeast Candida albicans by the contact method either (images not shown). Therefore, 3 of these 4 advanced materials showed positive antimicrobial results against Gram-positive and Gram-negative bacteria and thus could be very useful for many bioengineering applications with high antibacterial activity requirements. However, none of the 4 materials were able to inhibit the yeast growth.

Discussion

The antimicrobial activity of new advanced materials can be analyzed by this easy-to-follow protocol consisting of 2 complementary procedures based on 2 existing methods: the agar disk diffusion test³⁸ and the antimicrobial activity measured on material surfaces according to the ISO 22196:2007 norm³⁹.

In this research field, many of the antimicrobial tests reported in the literature are highly assay-dependent. Therefore, it is very important to have detailed and consistent protocols in place across laboratories. This article is a step in that direction. Furthermore, it could be very helpful for many researchers who are less experienced in this field and require in-depth, step-by-step procedures to follow for accurate results.

This protocol can be used with many types of materials cut into disk shapes of 10-mm diameter. Brittle materials can be swollen in a suitable solvent for 1 h to render the cutting process easier. Thus, hydrophilic materials such as alginates can be hydrated in autoclaved distilled water. Other solvents, such as ethanol, ketone, and dichloromethane, can be employed to swell hydrophobic materials for 1 h before cutting them. However, some materials such as poly(3-hydroxybutyrate-co-3-hydroxyvalerate) do not need to be swollen and they can be cut directly. After that, it is very important to dry the sample material disks in a vacuum oven and sterilize each specimen with ethanol and UV radiation for 1 h to avoid any contamination risk.

This protocol recommends TSA and TSB as culture media and the use of pure cultures of 3 microorganisms to reach a broad range of microorganisms: the Gram-positive bacteria Staphylococcus aureus, the Gram-negative bacteria Escherichia coli, and the yeast Candida albicans. However, alternative culture media and other microorganisms in need of different incubation conditions could also be used with this protocol. Sometimes, only 1 microorganism is tested to have an initial idea of the antimicrobial activity of a new material.

The materials showing strong antimicrobial activity against the recommended 3 different types of microorganisms should also be tested against antibiotic-resistant pathogens such as methicillin-resistant Staphylococcus epidermidis (MRSE), which have been successfully utilized with this protocol. Other important drug-resistant microorganisms which are causing much concern are the Gram-positive methicillin-resistant Staphylococcus aureus (MRSA) and vancomycin-resistant Enterococci (VRE), and the Gram-negative Pseudomonas aeruginosa^40,41.

Biofilm inhibition and the antimicrobial activity of materials against other types of microorganisms such as viruses and parasites cannot be tested with this protocol. However, this protocol provides a very useful starting point for an antimicrobial study of a new advanced material.

In the antimicrobial agar disk diffusion test, a critical step occurs when the sample disk has to be placed in the center of the plate because some materials fold as soon as they get in contact with the agar media. In this case, it is recommended to use a sterile pair of tweezers to carefully unfold the sample. On the other hand, in the contact method, it is critical to wash the control and sample disks very well with PBS by pipetting them four times followed by a vigorous vortexing and sonication in order to ensure that no viable microorganisms remain adhered to the material surface.

This video protocol can be utilized in many bioengineering applications, such as bioprocess engineering, tissue engineering, controlled drug delivery, packaging materials, wastewater treatment, and agriculture, which use biomaterials with a highly desirable antimicrobial capacity.

The results obtained with this protocol are qualitative (the images) and quantitative (the normalized width of the antibacterial "halo" and the loss of viability) with a good analysis of its reproducibility (mean ± standard deviation). When comparing different materials, these mean values obtained with the diffusion and contact method results analysis must be analyzed by one-way ANOVA, followed by Turkey's post hoc analysis, in order to study if they are, statistically, significantly different (p <0.01).

Materials

List of materials used in this article

Name	Company	Catalog Number	Comments
Cylindrical punch			10 mm diameter
Petri dishes	soria genlab	P101	90 mm diameter, sterile
Tryptic soy agar (TSA)	Liofilchem	610052	Dehydrated medium 500 g (powder)
Tryptic soy broth (TSB)	Liofilchem	610053	Dehydrated medium 500 g (powder)
Sterile cotton swab	EUTOTUBO	300200
Centrifuge tubes	VIDRA FOC, SA	429900	50 mL, sterile
Ethanol	VWR	83813360	Absolute ethanol
Sterile 48-wells plate	COSTAR	3548	Flat bottom with lid, tissue culture treated, non-pyrogenic, polystyrene
A pair of tweezers	BRAUN	24612036	Toothless
Sterile phosphate buffered saline (PBS).	VWR	E404-100TAPBS
Vaccum oven with a connected vacuum pump	JP Selecta, SA	5900620
Laminar flow hood	TELSTAR Technologies, SL	TELSTAR AH-100	12.0 W lamp of UV-C radiation
Class II Biological safety cabinet	LABOGENE	MARS 1200
Incubator	ASTEC CO, LTD	SCA-165DR
Vortex mixer	Biosan	V-1 Plus
Spectrophotometer	Macherey-Nagel, Germany	Nanocolor UV/VIS II
Bunsen burner	JP Selecta, SA	7001539
Alcohol burner	VIDRA FOC, SA	1658/20	In case sterilisation is necessary to be performed inside class II biological safety cabinet
Orbital shaker	sartorius stedim	8864845
Sonicator	SELECTA	3000617	50/60 Hz
Digital calliper	ACHA	17-260	0-150 mm
Serological pipette	Fisherbrand	13-678-11	25 mL, sterile
Serological pipette	VWR	612-4950	5 mL, sterile
Serological pipette	VWR	612-5541	10 mL, sterile
Micropipette	GILSON	FA10005P	Pipetman L P200L, plastic 20-200 µL
Micropipette	GILSON	F123602	Pipetman P1000, 200-1000 µL
Micropipette	GILSON	FA10016	Pipetman L P12X300L, 20-300 µL
Micropipette tips	LABBOX	TIBP-200-960	2-200 µL
Micropipette tips	LABBOX	TIBP-1K0-480	100-1000 µL
Pre-sterilized tube	INSULAB	301402	10 mL
Photo camera	Canon EOS 5D		Any camera with high resolution can also be utilized
Gram-positive bacteria Staphylococcus aureus		strain V329	Cucarella et al. J Bacteriol 183 (9),  2888–2896 (2001)
Gram-negative bacteria Escherichia coli	Colección Española de Cultivos Tipo CECT	CECT 101
Yeast Candida albicans	Colección Española de Cultivos Tipo CECT	CECT 1394
Microcentrifuge tubes	DASLAB	175508	1,5 mL
Autoclave	JP Selecta, SA	4002136
Spectrophotometer-cuvettes	UVAT Bio CB	F-0902-02	4,5 mL
Drigalski spatula	LABBOX	SPRP-L05-1K0	Sterile, disposable
glass balls (2 mm diameter)	Hecht Karl	1401/2	Autoclavable, alternative device to the Drigalski spatula
Autoclave bags	DELTALAB	200318	To sterilize microbiological residues or contaminated material
Electronic pipette filling device	JetPip	JET BIOFIL
Laboratory bottle with ISO thread, graduated, borosilicate 3.3	LABBOX	SBG3-100-010	100 mL, for autoclaving culture media
Laboratory bottle with ISO thread, graduated, borosilicate 3.3	LABBOX	SBG3-250-010	250 mL, for autoclaving culture media
Laboratory bottle with ISO thread, graduated, borosilicate 3.3	LABBOX	SBG3-500-010	500 mL, for autoclaving culture media
Laboratory bottle with ISO thread, graduated, borosilicate 3.3	LABBOX	SBG3-1K0-010	1000 mL, for autoclaving culture media
Latex gloves	DENIA	2278000000
Indicator tape for sterilization	LABBOX	STAP-A55-001	Self-adhesive tape with impregnated paper turning to colour when exposed to sterilization process.
Universal test tube rack	LABBOX	MTSP-001-001	To hold centrifuge tubes
Microcentrifuge tube rack	VWR	211-0210	To hold microcentrifuge tubes
Sterile loop	ACEFE S.A.	100140055	10 µL of capacity for microbial culture
Material M1	Universidad Católica de Valencia San Vicente Mártir (UCV)		Material type 1
Material M2	Universidad Católica de Valencia San Vicente Mártir (UCV)		Material type 2
Material M3	Universidad Católica de Valencia San Vicente Mártir (UCV)		Material type3
Material M4	Universidad Católica de Valencia San Vicente Mártir (UCV)		Material type 4
Material C	Universidad Católica de Valencia San Vicente Mártir (UCV)		Control material