Direct and Indirect Culture Methods for Studying Biodegradable Implant Materials In Vitro

Podsumowanie

We introduce three methods of direct culture, direct exposure culture, and exposure culture for evaluating the in vitro cytocompatibility of biodegradable implant materials. These in vitro methods mimic different in vivo cell-implant interactions and can be applied to study various biodegradable materials.

Streszczenie

Over the past several decades, biodegradable materials have been extensively explored for biomedical applications such as orthopedic, dental, and craniomaxillofacial implants. To screen biodegradable materials for biomedical applications, it is necessary to evaluate these materials in terms of in vitro cell responses, cytocompatibility, and cytotoxicity. International Organization for Standardization (ISO) standards have been widely utilized in the evaluation of biomaterials. However, most ISO standards were originally established to assess the cytotoxicity of nondegradable materials, thus providing limited value for screening biodegradable materials.

This article introduces and discusses three different culture methods, namely, direct culture method, direct exposure culture method, and exposure culture method for evaluating the in vitro cytocompatibility of biodegradable implant materials, including biodegradable polymers, ceramics, metals, and their composites, with different cell types. Research has shown that culture methods influence cell responses to biodegradable materials because their dynamic degradation induces spatiotemporal differences at the interface and in the local environment. Specifically, the direct culture method reveals the responses of cells seeded directly on the implants; the direct exposure culture method elucidates the responses of established host cells coming in contact with the implants; and the exposure culture method evaluates the established host cells that are not in direct contact with the implants but are influenced by the changes in the local environment due to implant degradation.

This article provides examples of these three culture methods for studying the in vitro cytocompatibility of biodegradable implant materials and their interactions with bone marrow-derived mesenchymal stem cells (BMSCs). It also describes how to harvest, passage, culture, seed, fix, stain, characterize the cells, and analyze postculture media and materials. The in vitro methods described in this article mimic different scenarios of the in vivo environment, broadening the applicability and relevance of in vitro cytocompatibility testing of different biomaterials for various biomedical applications.

Wprowadzenie

For decades, biodegradable materials have been extensively studied and used in biomedical applications such as orthopedic^1,2, dental^3,4, and craniomaxillofacial⁵ applications. Unlike permanent implants and materials, biodegradable metals, ceramics, polymers, and their composites gradually degrade in the body over time via different chemical reactions in the physiological environment. For example, biodegradable metals such as magnesium (Mg) alloys^1,6,7 and zinc (Zn) alloys^8,9 are promising materials for bone fixation devices. Their biodegradability could eliminate the necessity for secondary surgeries to remove the implants after bone healing. Biodegradable ceramics such as calcium phosphate cements (CPCs) have shown exciting potential for the treatment of osteoporotic vertebral compression fractures in percutaneous kyphoplasty¹⁰. The CPCs provide mechanical support for the fractured vertebral body and gradually degrade after the fracture has healed.

Biodegradable polymers, such as some polysaccharides and polyesters, have also been widely explored for biomedical applications. For instance, chitosan hydrogel as a biodegradable polysaccharide has exhibited its capabilities for preventing infection and regenerating skin tissue¹¹. Poly-L-lactic acid (PLLA), poly(glycolic acid) (PGA), and poly(lactic-co-glycolic acid) (PLGA) are widely studied polyesters for fabricating 2D or 3D porous scaffolds for tissue engineering applications^12,13,14. Moreover, composite materials integrate two or more phases of metals, ceramics, and polymers to provide advanced functions for a wide range of biomedical applications^15,16,17. For example, PLGA and calcium phosphate composites can be used to fabricate biodegradable scaffolds for applications such as repairing skull bone defects¹⁸. These biodegradable scaffolds and implants could support and promote the growth of cells and tissues and then gradually degrade in the body over time.

As shown in Supplemental Table 1, different biodegradable materials may have varied degradation mechanisms, products, and rates. For example, magnesium alloys, such as Mg-2 wt % Zn-0.5 wt % Ca (ZC21)¹, Mg-4 wt% Zn-1 wt% Sr (ZSr41)¹⁹, and Mg-9 wt% Al-1 wt% Zinc (AZ91)²⁰, degrade by reacting with water, and their degradation products mainly include Mg²⁺ ions, OH^- ions, H₂ gas, and mineral depositions. The degradation rate for biodegradable metals varies depending on their different compositions, geometries, and degradation environments. For example, Cipriano et al.¹⁹ reported that ZSr41 wires (Ø1.1 × 15 mm) lost 85% mass while pure Mg wires with the same geometry lost 40% mass after being implanted in the rat tibiae for 47 days. Biodegradable ceramic materials such as hydroxyapatite (HA) and β-tricalcium phosphate (β-TCP) can degrade via solution-driven extracellular liquid dissolution or break down into small particles and then degrade via both extracellular liquid dissolution and cell-mediated resorption processes. The degradation products of these calcium phosphate-based ceramics may include Ca²⁺ ions, (PO₄)^3- ions, OH^- ions, and mineral depositions²¹. The degradation rate for calcium phosphate ceramics is significantly affected by their crystal structures. For instance, Van Blitterswijk et al.²² reported that HA with 40 vol.% micropores did not lose any mass while β-TCP with 40 vol.% micropores lost 30 ± 4% mass after being implanted in the tibiae of rabbits for 3 months. Polymers such as PLGA^14,23 may degrade due to hydrolysis of the ester linkages in the presence of water, and the degradation products mainly include lactic and glycolic acids. It may take one month for PLGA 50/50 and several months for PLGA 95/5 to achieve complete degradation²⁴.

Cell response and cytocompatibility testing are critical to evaluate and screen these biodegradable implant materials for biomedical applications. However, current standards from the International Organization for Standardization (ISO), such as ISO 10993-5:2009 "Biological evaluation of medical devices-Part 5 Tests for in vitro cytotoxicity", were initially designed to assess the cytotoxicity of nondegradable biomaterials such as Ti alloys and Cr-Co alloys in vitro²⁵. Specifically, ISO 10993-5:2009 only covers the in vitro cytotoxicity tests of the extract, direct contact, and indirect contact tests. In the extract test, the extract is prepared by immersing samples in extraction fluids such as culture media with serum and physiological saline solutions under one of the standard time and temperature conditions. The collected extract or dilution is then added into the cell culture to study cytotoxicity. For the direct contact test, direct contact between sample and cells is achieved by placing the test sample on the established (adhered) cell layer. In the indirect contact test, the culture media containing serum and melted agar is pipetted to cover the established cells. The sample is then placed onto the solidified agar layer with or without a filter.

The ISO standards have shown some limitations when applied to evaluate biodegradable materials in vitro. Unlike nondegradable materials, the degradation behaviors of biodegradable materials are dynamic and may change at a different time or in varied environmental conditions (e.g., temperature, humidity, media composition, and cell type). The extract test only evaluates the cytotoxicity of the degradation products of the material and does not reflect the dynamic process of sample degradation. Both direct and indirect contact tests of the ISO standard only characterize the interactions between the established cells and samples. Moreover, in the indirect contact test, the materials and cells are in different microenvironments that do not reflect the in vivo environment and do not capture the dynamic degradation of biodegradable materials.

The objective of this article is to introduce and discuss the cytocompatibility testing methods for various biodegradable implant materials to address the abovementioned limitations of the methods described in the current ISO standards. The methods presented in this article consider the dynamic degradation behavior of implant materials and the different circumstances of cell-material interactions in vivo. Specifically, this article provides three cytocompatibility testing methods, namely direct culture, direct exposure culture, and exposure culture for various biodegradable materials, including biodegradable polymers, ceramics, metals, and their composites for medical implant applications.

In the direct culture method, cells suspended in the culture media are directly seeded on the samples, thus evaluating the interactions between newly seeded cells and the implants. In the direct exposure culture, the samples are placed directly on the established cell layer to mimic the interactions of implants with established host cells in the body. In the exposure culture, the samples are placed in their respective well inserts and then introduced to the culture wells with established cells, which characterizes the responses of established cells to the changes in the local environment induced by implant degradation when they have no direct contact with implants. The direct culture and direct exposure culture methods evaluate the cells directly or indirectly in contact with the implant materials in the same culture well. The exposure culture characterizes the cells indirectly in contact with the implant materials within a prescribed distance in the same culture well.

This article presents a detailed description of the cytocompatibility testing for different biodegradable materials and their interactions with model cells, that is, bone marrow-derived mesenchymal stem cells (BMSCs). The protocols include the harvesting, culturing, seeding, fixing, staining, and imaging of the cells, along with analyses of postculture materials and media, which apply to a variety of biodegradable implant materials and a wide range of cell types. These methods are useful for screening biodegradable materials for different biomedical applications in terms of cell responses and cytocompatibility in vitro.

Protokół

This protocol was approved by the Institutional Animal Care and Use Committee (IACUC) at the University of California at Riverside (UCR) for cell and tissue harvesting. A 12-week-old female Sprague-Dawley (SD) rat is shown as an example in the video. Younger female and male rats are preferred.

1. Cell culture preparation

NOTE: The three culture methods described in this article are generally applicable for different cell types that are adherent. Here, BMSCs harvested from rat weanlings will be introduced as an example for cell culture preparation. Depending on their relevance for specific medical applications, different cell types may be utilized, including primary cells harvested from animals or human donors and cell lines from a cell/tissue bank.

1. Harvesting BMSCs from rat weanlings
   NOTE: The schematic diagram in Figure 1 shows the steps to harvest BMSCs from rat weanlings.
   1. Euthanize the Sprague Dawley (SD) rat by CO₂ inhalation.
   2. Remove the skin and muscle and connective tissues to dissect the femur out of the euthanized rat. Place the femoral bones in a 15 mL conical tube (polypropylene) containing cell culture medium. Place the conical tubes on ice until the time of performing cell extraction.
      NOTE: Tibia also can be used to harvest BMSCs. The cell culture medium is Dulbecco's Modified Eagle Medium (DMEM) supplemented with 10% fetal bovine serum (FBS) and 1% penicillin/streptomycin (P/S).
   3. Transfer the bones to a Petri dish in the biological safety cabinet. Cut the ends of the bone using a surgical blade and flush the bone marrow into a 50 mL conical tube (polypropylene) by washing the bone marrow cavity with cell culture media using a syringe with a 25½ G needle.
      NOTE: Insert a syringe with an 18 G needle into the media with bone marrow. Slowly and gently, take up and dispense the media to break apart the large chunk of marrow until no visible cell/tissue agglomerates are present.
   4. Filter the cell suspension using a 70 µm filter, followed by centrifugation at 126 × g (1,000 rpm) for 5 min to get the cell pellets.
   5. Aspirate the supernatant media and replenish with 10 mL of fresh media. Gently pipette up and down to resuspend the cells using a 10 mL serological pipette.
   6. Pipette the suspension directly on the inside bottom of a T-75 flask and add media to bring the volume up to 25 mL. Culture the cells in an incubator in a standard sterile cell culture environment (i.e., 37 °C, humidified atmosphere with 5% CO₂ and 95% air).
   7. After 3-7 days, rinse away the nonadherent cells by aspirating the old medium and replenishing with fresh medium. Continue culturing and feeding the cells with fresh medium until they are ready for cell passage, freezing, or use in an experiment.
2. Cell maintenance
   1. Change the cell culture medium regularly to remove cellular waste products and replenish the nutrients approximately every other day until the cells are 90%-100% confluent. At 90% confluency, passage, freeze, or use the cells in an experiment.
   2. Passaging cells
      NOTE: Passaging, also referred to as subculturing, is a term that applies whenever cells are transferred from one culture to another. Freshly harvested cells are at passage stage 0 (P₀). The amounts of trypsin-ethylenediaminetetraacetic acid solution (trypsin-EDTA) and media described in this article are for a T-75 flask.
      1. Check the cells under an optical microscope to confirm that the cells are 90% confluent.
      2. Aspirate the medium from the cell flask.
      3. Dispense 10 mL of phosphate-buffered saline (PBS) into the flask using a serological pipette. Gently rock the flask to rinse the cells with PBS; aspirate all the PBS.
         NOTE: This step serves as an extra rinse to ensure that no dead cells or cellular waste will be transferred during passaging.
      4. Dispense 3 mL of trypsin-EDTA into the cell flask directly onto the surface of the cells. Gently rock the flask to ensure the entire surface with the cells is covered by the trypsin-EDTA.
      5. Place the cell flask with trypsin-EDTA into the incubator for 5 min to allow the cells to detach.
      6. After 5 min in the incubator, check the cells under an optical microscope to confirm that the cells are detached. If some cells have not detached, tap the side of the cell flask gently, and check the flask again.
      7. Add 9 mL of fresh medium to the cell flask to dilute the trypsin-EDTA. This provides more accessible proteins for the trypsin-EDTA to bind to instead of lysing the cells.
      8. Pipette out the cells in media and trypsin-EDTA and dispense them into a 15 mL conical tube. Centrifuge the cells at 126 × g (1,000 rpm) for 5 min.
      9. Without disturbing the cell pellet, aspirate the medium with trypsin-EDTA.
      10. Add 5-10 mL of fresh media to the centrifuge tube and gently resuspend the cells in the medium using a 10 mL serological pipette.
      11. Pipette the cells suspended in medium out of the centrifuge tube and split the volume into 2-3 fresh culture flasks. Add enough medium to bring the total medium volume to 25 mL for each flask.
          ​NOTE: The split ratio during subculture may vary depending on the cell types and specific growth characteristics.
      12. Check the cells under an optical microscope and place them back into the incubator.
   3. Freezing cells
      1. Check the cells under an optical microscope to confirm that the cells are 90% confluent.
      2. Repeat steps 1.2.2.2 to 1.2.2.9.
      3. Add 900 µL of fresh medium to the centrifuge tube with a 100-1000 µL micropipette. Slowly and gently resuspend cells in medium using the same micropipette.
      4. Transfer the 900 µL cell suspension into a cryovial. Add 100 µL of dimethylsulfoxide (DMSO).
      5. As soon as possible, place the cryovial into a cylindrical foam container designed to regulate temperature decrease (see the Table of Materials). Place the foam container in the -80 °C freezer.
   4. Thawing cells
      1. Thaw the frozen cells in the water bath. Take a sterile 15 mL conical tube filled with 5 mL of fresh medium, place the cells in the conical tube, and centrifuge at 126 × g (1,000 rpm) for 5 min.
      2. Aspirate the medium containing DMSO.
      3. Add 5-10 mL of fresh medium to the 15 mL conical tube of cells. Slowly and gently pipette up and down to resuspend the cells.
      4. Pipette the cells suspended in medium out of the 15 mL conical tube and dispense into a new T-75 flask. When dispensing cells, use a sweeping motion to distribute the cells as evenly as possible on the bottom of the cell flask.
      5. Add enough fresh medium to bring the total medium volume to 25 mL for each T-75 flask.
      6. Check the cells under an optical microscope and place the cell flask back into the incubator.

2. Sample preparation and sterilization

1. Sample preparation
   1. Use tissue-culture-treated plates such as 6, 12, 24, 48, or 96-well plates for cell culture experiments described in this article. Select the type of tissue-culture plates and the volume of medium in each well based on different experimental designs such as sample dimension.
2. Sterilize or disinfect all the biodegradable samples before the cell culture.
   NOTE: Disinfection is acceptable for in vitro studies when the samples are prone to chemical and/or surface changes under some sterilization conditions involving high heat, oxidizer, and/or radicals. Sterilization or disinfection methods for different sample types vary depending on the different properties of the materials, such as polymers, metals, and ceramics. The process for sterilization or disinfection could involve heat, gas, radiation, chemicals, high pressure, or a combination of these.
   1. Biodegradable metals
      1. In general, use ultraviolet (UV) radiation to disinfect biodegradable metals for in vitro studies.
         NOTE: For example, Zhang et al. reported that pure magnesium (Mg) and ZC21 Mg alloy samples were disinfected under UV radiation for 4 h before they were utilized in the cell studies¹. For in vivo studies, the samples are generally required to be sterilized. For many biodegradable metals such as magnesium or magnesium alloys, autoclaving using steam should be avoided because these samples could be oxidized or corroded in water⁶. A quartz dish is recommended for UV disinfection because it provides better UV transparency than most glasses and plastics.
      2. Sterilize Mg alloy samples under dry heat in an oven or autoclave at the temperature range of 100-200 °C.
         NOTE: As some metallic alloys could still become oxidized on the surface at high temperatures in the air, high-intensity radiation may be used as an alternative in some cases. However, high-intensity radiation such as alpha or gamma radiation should be avoided when sterilizing thin metallic foils. It may cause atom displacement within the materials, changing the microstructure of materials.
      3. Use ethylene oxide (EtO) gas sterilization as an alternative method for biodegradable metals sensitive to heat and radiation²⁶.
   2. Biodegradable ceramics
      1. Generally, disinfect biodegradable ceramics using UV radiation or 70% ethanol solution before in vitro studies.
         NOTE: For example, Liu et al. reported that the calcium phosphate samples were disinfected via immersion in 70% ethanol for 1 h and exposure to UV light for 12 h on each side before they were used in in vitro cytocompatibility tests²⁷.
      2. Use autoclaves to sterilize biodegradable ceramics if high temperature and water vapor do not damage their compostions and microstructures.
         NOTE: Some ceramics might be affected by autoclaving. For example, phase change and surface roughening were found when yttria-stabilized zirconia ceramics were autoclaved at 121 °C for 15 min. Additionally, CPCs cannot be sterilized via autoclaving with steam because the samples will react with water.
      3. Use alternative sterilization methods such as Cobalt-60 radiation for the abovementioned yttria-stabilized zirconia ceramics and CPC samples²⁸.
   3. Biodegradable polymers
      1. In general, disinfect biodegradable polymers using UV radiation or 70% ethanol before using them in cell studies in vitro.
         NOTE: Some polymers may undergo chemical changes under UV radiation. For sterilization, gamma-ray treatment such as Cobalt-60 radiation may be used. For example, starch powders were sterilized under Cobalt-60 radiation before being utilized in in vitro cell studies²⁹.
      2. Autoclave polymer materials that can withstand high temperature and moisture.
         NOTE: For instance, polymers such as polypropylene can be autoclaved as they can tolerate autoclaving temperatures (i.e., 121-134 °C). Some polymers such as polycaprolactone (PCL) cannot be autoclaved because of their relatively low melting points (i.e., around 60 °C)³⁰.
      3. Use EtO gas to sterilize polymeric materials sensitive to heat or radiation sterilization.

3. Cell culture methods

1. Direct culture methods
   NOTE: The schematic diagram in Figure 2A shows the steps of the direct culture method. In this article, BMSCs were cultured on a Mg-derived plate placed inside the wells of a 12-well tissue-culture-treated plate as an example to illustrate the culture method.
   1. Follow the steps described in steps 1.2.2.1-1.2.2.10 to obtain the cell suspension.
   2. Use a 90% confluent flask to determine the cell concentration in the cell suspension using a hemocytometer. Dilute the cell suspension using fresh medium to a prescribed cell concentration needed for the cell study in vitro.
      NOTE: The seeding density of cells is determined by the experimental design. For example, cell densities of 2,000-40,000 cells/cm² have been used in different cell studies with biodegradable materials.
   3. Place the samples (Mg plate) in the center of the 12-well treated tissue-culture plates. Sequentially, rinse the culture plates with 2 mL of PBS and 2 mL of DMEM to calibrate the osmotic pressure under sterile conditions. Add 3 mL of the diluted cell suspension into each well onto the samples of interest.
   4. Culture the cells in an incubator under standard cell culture conditions for 24 h.
      NOTE: The culture time may be longer or shorter than 24 h depending on the experimental design.
2. Direct exposure cultures
   NOTE: The schematic diagram in Figure 2B shows the steps of direct exposure culture.
   1. As described in steps 3.1.1 and 3.1.2, prepare the cell suspension with the required concentrations of cells based on the experimental design for different cell types and intended applications.
   2. Rinse the culture plates with 2 mL of PBS and 2 mL of DMEM sequentially to calibrate the osmotic pressure under sterile conditions. Add 3 mL of the diluted cell suspension into each well. Culture the cells in the humidified incubator under standard cell culture conditions for 24 h or until the cells reach 50-80% confluence.
      NOTE: The cell confluence level may vary for different cell types and experimental design.
   3. After 24 h, rinse the cells in the well plate with PBS using a pipette to remove floating dead cells.
   4. Place the disinfected or sterilized samples directly on the adhered cells. Add 3 mL of fresh medium into each well.
   5. Culture the cells under standard cell culture conditions for another 24 h.
      NOTE: The culture time may be longer or shorter than 24 h depending on the experimental design.
3. Exposure cultures
   NOTE: The schematic diagram in Figure 2C shows the steps of the exposure culture method.
   1. Initial steps for the cell preparation are the same as the exposure culture. As described in steps 3.1.1 and 3.1.2, prepare the cell suspension with the desired cells. Similar to steps 3.2.1 and 3.2.2, seed the cells in the well plate at the desired density and culture them in an incubator under standard cell culture conditions for 24 h.
   2. After 24 h, rinse the adherent cells with PBS to remove floating dead cells, followed by the addition of 3 mL of fresh medium into each well.
   3. Afterwards, place the samples in the well inserts with a membrane pore size of 0.4 µm and place the well inserts with the samples into each well with the cells.
   4. Culture the cells under standard cell culture conditions for another 24 h.
      ​NOTE: The culture time may be longer or shorter than 24 h depending on the experimental design.

4. Postculture characterization of cells

NOTE: For direct culture and direct exposure culture, fix, stain, image, and analyze the cells adherent on both well plates and samples. For exposure culture, analyze the cells adhered to the well-plates.

1. Cell fixation
   1. Collect the postculture medium from each well into a corresponding 15 mL conical tube for further analysis. Collect all the samples after culture for further analysis.
   2. Rinse the cells adherent on both samples and well plates 3 times using PBS.
   3. Add 1 mL of 4% paraformaldehyde (PFA, 10% neutral buffered formalin) into each well plate. Put the lid back on the well plate and allow the PFA to react for 20 min.
   4. After 20 min, aspirate the PFA and dispense it into a waste bottle. Rinse the well plate 3 times using PBS to remove the PFA, and transfer the waste to the waste bottle.
2. Cell staining
   1. Prepare the working stocks of the staining agents following the manufacturers' instructions.
      NOTE: For example, Alexa Fluor 488 Phalloidin is used to stain F-actin, and 4′, 6-diamidino-2-phenylindole (DAPI) is used to stain cell nuclei. Staining time may be reduced if the samples degrade rapidly in the staining solutions.
   2. Add 200-400 µL of diluted Alexa Fluor 488 Phalloidin staining agent to each well to cover the cells on the well plate and the sample. Wrap the well plate in aluminum foil to prevent light exposure, and allow the Alexa Fluor 488 Phalloidin to react for 20 min at room temperature.
   3. Collect the Alexa Fluor 488 Phalloidin staining agent and dispense it into the corresponding waste bottle. Rinse the well plate 3 times using PBS to remove the excess Alexa Fluor 488 Phalloidin, and dispense the used PBS into the corresponding waste bottle.
   4. Add 200-400 µL of diluted DAPI to each well to cover the cells in the well and on the sample. Wrap the well plate in aluminum foil and allow the DAPI to react for 5 min at room temperature.
   5. Collect the DAPI and dispense it into the corresponding waste bottle. Rinse the well plate 3 times using PBS to remove the DAPI, and dispense the used PBS into the corresponding waste bottle.
3. Cell imaging
   1. After staining, image the cells using a fluorescence microscope. Whenever possible, take phase-contrast images of cells in addition to fluorescence images. Image the cells on the biodegradable samples as soon as possible or immediately after staining to avoid or reduce possible changes caused by the continuous degradation of samples. Store the cells in the well plates in a buffer solution at 2-8 °C after fixation, and image the cells as soon as possible after staining to avoid the loss of fluorescence signals.
   2. For direct culture and direct exposure culture, image and evaluate two types of cells: (1) the cells on the samples (in direct contact with the samples) and (2) the cells adherent on the well plate surrounding the samples (indirect contact with the samples), as shown in Figure 3A.
   3. For exposure culture, as shown in Figure 3B, use an image guide when taking the fluorescence images of cells to determine if the cell response would be different in response to the dynamic degradation gradient of the samples. Image and analyze the cells located in the area within the inner ring (3.5 mm away from the center) and the outer ring (7 mm away from the center) separately.
      NOTE: The image guide is used to define the distance between the cells and samples.
   4. For each sample and well in the culture plates, randomly take at least five images from each area of interest where the cells are either in direct contact or indirect contact with the samples at a predefined distance.
4. Image analysis
   1. For all the cell images obtained from step 4.3, quantify the cell morphology by measuring the cell spreading area and aspect ratio using software such as ImageJ for image analysis.
   2. Count the number of cells in each image area. Calculate the cell adhesion density under direct and indirect contact conditions as the number of cells per unit area.

5. Postculture analyses of media and samples

1. Measure the pH of postculture medium.
   NOTE: Some samples change the pH value of the medium during their degradation. For example, biodegradable metals such as magnesium alloys usually increase the pH value of the medium due to their degradation³¹. In contrast, biodegradable polymers such as PLGA often decrease the pH value of the medium when they degrade³². Measuring the pH value of postculture medium can indicate the degradation of these samples in vitro.
   1. Before cell fixation, collect the postculture medium as in step 4.1.1.
   2. Measure the pH values of the postculture medium in each well immediately after collection, using a precalibrated pH meter.
      NOTE: The pH of the media may drift over time because of environmental conditions such as CO₂ level and temperature, which should be taken into consideration.
2. Analyze the medium compositions for the degradation behavior of biodegradable samples. For some samples that cause a color change of the medium, measure the optical density (O.D.) value of the postculture medium using a spectrophotometer or a microplate reader to determine the degradation behavior. Alternatively, use ultraviolet-visible spectroscopy (UV-VIS) and Fourier transform infrared spectroscopy-attenuated total reflectance (FTIR-ATR) to analyze the degradation products in the postculture medium.
   NOTE: Measuring the degradation products in the post-culture medium is valuable for understanding the degradation behavior of the samples. One of the most common approaches is to measure the ions of interest in the postculture medium using an inductively coupled plasma-optical emission spectrometer (ICP-OES). The ICP-OES can be used to measure the compositions of postculture medium of metals and ceramics but may not be suitable for polymers. Polymers usually consist of carbon, hydrogen, and oxygen, and accurate quantification of these elements is difficult for ICP-OES.
   1. Following step 5.1.2 for pH measurement, collect and dilute the medium using a desirable dilution factor for optimal measurements of ion concentrations.
   2. Measure the concentrations of the ions of interest in the postculture medium using an ICP-OES.
3. Postculture analysis of samples
   NOTE: After in vitro cell study, the biodegradable samples may change in dimension, mass, surface morphology, microstructure, and composition. Postculture analysis of samples helps understand the degradation mechanism of samples.
   1. After cell culture, take the photographs of the samples to show possible changes in sample dimension, color, morphology, and other visible characteristics.
   2. Dry or dehydrate the postculture samples and measure the sample mass, dimension, and volume to quantify any changes in mass, dimension, and volume.
   3. Use a scanning electron microscope (SEM) to characterize the microstructure and morphology of the samples. Use energy dispersive X-Ray spectroscopy (EDX) and X-ray diffraction (XRD) to characterize the composition and phase of the degradation products on the samples. Use FTIR-ATR to detect the chemical bonding on the sample surfaces.

Wyniki

Figure 4 shows the representative fluorescence images of BMSCs under direct and indirect contact conditions using different culture methods. Figure 4A,B show the BMSCs under direct and indirect contact conditions after the same 24 h direct culture with ZC21 magnesium alloys¹. The ZC21 alloys consist of 97.5 wt% Magnesium, 2 wt% Zinc, and 0.5 wt% calcium. The cells that have no direct contact with the ZC21 alloy samples sp...

Dyskusje

Different cell culture methods can be used to evaluate the in vitro cytocompatibility of biomaterials of interest for various aspects of applications in vivo. This article demonstrates three in vitro culture methods, i.e., direct culture, direct exposure culture, and exposure culture, to mimic different in vivo scenarios where biodegradable implant materials are used inside the human body. The direct culture method is mainly used to evaluate the behavior of newly seeded cells directly ...

Materiały

Name	Company	Catalog Number	Comments
10 mL serological pipette	VWR	490019-704
12-well tissue-culture-treated plates	Thermo Fisher Scientific	353043
15 mL conical tube (Polypropylene)	VWR	89039-666
18 G needle	BD	305196
25½ G needle	BD	305122
4′,6-diamidino-2- phenylindole dilactate (DAPI)	Invitrogen	D3571
50 mL conical tube (Polypropylene)	VWR	89039-658
70 μm nylon strainer	Fisher Scientific	50-105-0135
Alexa Flour 488-phalloidin	Life technologies	A12379
Biological safety cabinet	LABCONCO	Class II, Type A2
Centrifuge	Eppendorf	Rotor F-35-6-30, Centrifuge5430
Clear Fused Quartz Round Dish	AdValue Technology	FQ-4085
CO2 incubator	SANYO	MCO-19AIC
CoolCell Freezer Container	Corning	432000	foam container designed to regulate temperature decrease
Cryovial	Thermo Fisher Scientific	5000-1020
Dimethyl Sulfoxide (DMSO)	Sigma-Aldrich	472301
Dulbecco’s modified Eagle’s medium (DMEM)	Sigma-Aldrich	D5648
EDX analysis software	Oxford Instruments	AztecSynergy
Energy dispersive X-ray spectroscopy (EDX)	FEI	50mm2 X-Max50 SDD
Fetal bovine serum (FBS)	Thermo Fisher Scientific Inc.	SH30910
Fluorescence microscope	Nikon	Eclipse Ti
Formaldehyde	VWR	100496-496
Hemacytometer	Hausser Scientific	3520
ImageJ software	National Institutes of Health and the Laboratory for Optical and Computational Instrumentation (LOCI, University of Wisconsin)
Inductively coupled plasma optical emission spectrometry (ICP-OES)	PerkinElmer	Optima 8000
Optical microscope	VWR	VistaVision
Penicillin/streptomycin (P/S)	Thermo Fisher Scientific, Inc.,	15070063
pH meter	VWR	model SB70P
Phosphate Buffered Saline (PBS)	VWR	97062-730
Scanning electronic microscope (SEM)	FEI	Nova NanoSEM 450
surgical blade	VWR	76353-728
Tissue Culture Flasks	VWR	T-75, MSPP-90076
Transwell inserts	Corning	3460
Trypsin-ethylenediaminetetraacetic acid solution (Trypsin-EDTA)	Sigma-Aldrich	T4049
X-ray diffraction instrument (XRD)	PANalytical	Empyrean Series 2