A Zebrafish Embryo Model for In Vivo Visualization and Intravital Analysis of Biomaterial-associated Staphylococcus aureus Infection


Your institution must subscribe to JoVE's Bioengineering section to access this content.

Fill out the form below to receive a free trial or learn more about access:


Enter your email below to get your free 10 minute trial to JoVE!

We use/store this info to ensure you have proper access and that your account is secure. We may use this info to send you notifications about your account, your institutional access, and/or other related products. To learn more about our GDPR policies click here.

If you want more info regarding data storage, please contact gdpr@jove.com.



The present study describes a zebrafish embryo model for in vivo visualization and intravital analysis of biomaterial-associated infection over time based on fluorescence microscopy. This model is a promising system complementing mammalian animal models such as mouse models for studying biomaterial-associated infections in vivo.

Cite this Article

Copy Citation | Download Citations

Zhang, X., de Boer, L., Stockhammer, O. W., Grijpma, D. W., Spaink, H. P., Zaat, S. A. A Zebrafish Embryo Model for In Vivo Visualization and Intravital Analysis of Biomaterial-associated Staphylococcus aureus Infection. J. Vis. Exp. (143), e58523, doi:10.3791/58523 (2019).


Biomaterial-associated infection (BAI) is a major cause of the failure of biomaterials/medical devices. Staphylococcus aureus is one of the major pathogens in BAI. Current experimental BAI mammalian animal models such as mouse models are costly and time-consuming, and therefore not suitable for high throughput analysis. Thus, novel animal models as complementary systems for investigating BAI in vivo are desired. In the present study, we aimed to develop a zebrafish embryo model for in vivo visualization and intravital analysis of bacterial infection in the presence of biomaterials based on fluorescence microscopy. In addition, the provoked macrophage response was studied. To this end, we used fluorescent protein-expressing S. aureus and transgenic zebrafish embryos expressing fluorescent proteins in their macrophages and developed a procedure to inject bacteria alone or together with microspheres into the muscle tissue of embryos. To monitor bacterial infection progression in live embryos over time, we devised a simple but reliable method of microscopic scoring of fluorescent bacteria. The results from microscopic scoring showed that all embryos with more than 20 colony-forming units (CFU) of bacteria yielded a positive fluorescent signal of bacteria. To study the potential effects of biomaterials on infection, we determined the CFU numbers of S. aureus with and without 10 µm polystyrene microspheres (PS10) as model biomaterials in the embryos. Moreover, we used the ObjectJ project file "Zebrafish-Immunotest" operating in ImageJ to quantify the fluorescence intensity of S. aureus infection with and without PS10 over time. Results from both methods showed higher numbers of S. aureus in infected embryos with microspheres than in embryos without microspheres, indicating an increased infection susceptibility in the presence of the biomaterial. Thus, the present study shows the potential of the zebrafish embryo model to study BAI with the methods developed here.


A variety of medical devices (referred to as "biomaterials") are increasingly used in modern medicine to restore or replace human body parts1. However, the implantation of biomaterials predisposes a patient to infection, called a biomaterial-associated infection (BAI), which is a major complication of implants in surgery. Staphylococcus aureus and Staphylococcus epidermidis are two most prevalent bacterial species responsible for BAI2,3,4,5,6. Implanted biomaterials form a surface susceptible to bacterial biofilm formation. Moreover, local immune response may be deranged by the implanted biomaterials, causing reduced effectiveness of bacterial clearance. The initial clearance of infecting bacteria is performed mainly by infiltrating neutrophils, which have strongly reduced bactericidal capacity in the presence of an inserted or implanted biomaterial7. Moreover, macrophages infiltrating the tissue after the initial influx of neutrophils will phagocytose the remaining bacteria but cannot effectively kill them intracellularly, due to deranged immune signaling that is a consequence of the combined presence of the biomaterial and bacteria8. Thus, the presence of biomaterials can facilitate intracellular survival of bacteria9,10,11,12,13 and biofilm formation on the implanted biomaterials4,14. Consequently, BAI may lead to the failure and need for replacement of implanted biomaterials, causing increased morbidity and mortality and prolonged hospitalization with additional costs2,15.

An increasing number of anti-BAI strategies are being developed2,16,17. In vivo evaluation of the efficacy of these strategies in relevant animal models is essential. However, traditional experimental BAI animal models (e.g., mouse models) are usually costly, time-consuming, and therefore not suitable for high throughput testing of multiple strategies18. Recent development of bio-optical imaging techniques based on bioluminescent/fluorescent labeling of host cells and bacteria may allow for the continuous monitoring of BAI progression and host-pathogen/host-material interactions in single small animals such as mice18,19,20,21. However, this technique is relatively complex and still in its infancy, and several issues must be addressed for quantitative analysis of BAI18. For instance, a high challenge dose is required to visualize bacterial colonization. In addition, light scattering and adsorption of bioluminescence/fluorescence signals in tissues of mammalian test animals must also be addressed18,19,21. Therefore, novel, cost-effective animal models allowing for intravital visualization and quantitative analysis over time are valuable complementary systems for studying BAI in vivo.

Zebrafish (embryos) have been used as a versatile in vivo tool for dissecting host-pathogen interactions and infection pathogenesis of several bacterial species such as mycobacteria22, Pseudomonas aeruginosa23, Escherichia coli24, Enterococcus faecalis25, and staphylococci26,27. Zebrafish embryos have many advantages such as optical transparency, a relatively low maintenance cost, and possession of an immune system highly similar to that in mammals28,29. This makes zebrafish embryos a highly economic, living model organism for intravital visualization and analysis of infection progression and associated host responses28,29. To allow visualization of cell behavior in vivo, transgenic zebrafish lines with different types of immune cells (e.g., macrophages and neutrophils) and even with fluorescently tagged subcellular structures have been developed28,29. In addition, the high reproduction rate of zebrafish provides the possibility of developing high throughput test systems featuring automated robotic injection, automated fluorescence quantification, and RNA sequence analysis27,30.

In the present study, we aimed to develop a zebrafish embryo model for biomaterial-associated infection using fluorescence imaging techniques. To this end, we developed a procedure to inject bacteria (S. aureus) in the presence of biomaterial microspheres into the muscle tissue of zebrafish embryos. We used S. aureus RN4220 expressing mCherry fluorescent protein (S. aureus-mCherry), which was constructed as described elsewhere for another S. aureus strain10,31. The transgenic zebrafish line (mpeg1: UAS/Kaede) expressing Kaede green fluorescent protein in the macrophages32 and blue fluorescent polystyrene microspheres were used. In a previous study, we have shown that intramuscular injection of microspheres into zebrafish embryos to mimic biomaterial implantation is feasible33. To quantitatively analyze the progression of BAI and associated cell infiltration in single embryos over time, we used the "Zebrafish-Immunotest" project file which is operated within "ObjectJ" (a plug-in for ImageJ) to quantify the fluorescence intensity of bacteria residing and macrophages infiltrating in the vicinity of the injection site of microspheres33. In addition, we determined the numbers of colony-forming units (CFU) of bacteria in the presence and absence of microspheres in the embryos to study potential effects of biomaterials on infection. Our present study demonstrates that with the methods developed here, the zebrafish embryo is a promising, novel vertebrate animal model for studying biomaterial-associated infections in vivo.

Subscription Required. Please recommend JoVE to your librarian.


In this protocol, maintenance of adult zebrafish is in compliance with the local animal welfare regulations as approved by the local animal welfare committee. Experiments with embryos were performed according to the 2010/63/EU Directive.

1. Preparation of "Bacteria-only" and Bacteria-microspheres Suspensions

NOTE: The S. aureus RN4220 strain expressing mCherry fluorescent protein (S. aureus-mCherry) is used. The S. aureus RN4220 strain is mutated in the virulence regulator gene agrA (accessory gene regulator A)34, and therefore may have relatively low virulence in the zebrafish embryo model. Other S. aureus strains or other bacterial species for BAI can be used.

  1. Take 4 to 5 colonies of S. aureus RN4220 bacteria from tryptic soya agar culture plates supplemented with 10 µg/mL chloramphenicol and culture the bacteria to mid-logarithmic growth phase in 10 mL of tryptic soy broth supplemented with 10 µg/mL chloramphenicol at 37 °C under shaking.
    1. During culture, dilute 100 µL of the bacterial suspension in 900 µL of sterile phosphate buffered saline (PBS) in a cuvette (width of 1 cm) for an optical density (OD) measurement at 620 nm (OD620). Culture the bacteria until the OD620 reaches 0.4–0.8.
      NOTE: An OD620 of 0.1 generally corresponds to 3.0 x 107 CFU/mL S. aureus. The OD620 of an inoculum of bacteria in mid logarithmic growth phase is between 0.4-0.8. Different time periods for culturing may be needed for other species and strains of bacteria.
  2. Centrifuge bacteria at 3,500 x g for 10 min and re-suspend the pelleted bacteria in 1 mL of sterile PBS. Subsequently wash the bacteria with sterile PBS 2 times, and finally re-suspend the bacteria in 1.1 mL of 4% (w/v) polyvinylpyrrolidone40 (PVP40) solution in PBS.
  3. Vortex this bacterial suspension and dilute 100 µL of the suspension in 900 µL of sterile PBS in a cuvette for the OD620 measurement. Adjust the concentration of the bacterial suspension with PVP40 solution. This is the "Bacteria-only" suspension.
  4. Biomaterials can be freely chosen to mix with bacterial suspension. In the present study, commercial polystyrene (PS) microspheres (blue fluorescent, 10 µm) are used. To generate a Bacteria-Microspheres suspension, centrifuge the microspheres for 1 min at 1,000 x g, room temperature, discard the supernatant and re-suspend the microspheres in the  “Bacteria-only” suspension (in PVP40 solution).
  5. In order to inject approximately equal doses of bacteria in the presence and in the absence of microspheres, the concentration of Bacteria-Microspheres suspension needs to be two thirds of the concentration of the “Bacteria-only” suspension (without microspheres). This is achieved by diluting the Bacteria-Microspheres suspension with 0.5 volume of PVP40 solution. Mix the suspensions by vortexing. Of note, this ratio (two thirds) has been assessed for S. aureus. It is also appropriate for S. epidermidis, but it is advised to check whether this ratio also applies to other bacterial species and other sizes (than 10 µm) or shapes of biomaterials (than microspheres) to be injected.
  6. Check the concentration of the “Bacteria-only” and Bacteria-Microspheres suspension by quantitative culture of 10-fold serial dilutions as below: transfer 100 µL of the suspensions to a 96 well-plate and serially dilute by transferring 10 µL aliquots of the suspension into 90 µL of sterile PBS. Plate duplicate 10 µL aliquots of the undiluted and diluted suspensions on agarose plates, incubate the plates at 37 °C overnight, count the colonies and calculate the numbers of bacteria (colony-forming units. CFU).

2. Breeding, Harvesting, and Maintenance of Zebrafish Embryos

  1. Follow the general procedures described earlier35,36 for breeding, harvesting, and maintenance of zebrafish embryos, with modifications described below. Cross a family of wild type Tupfel long fin (TL) zebrafish or zebrafish of the selected transgenic line (here, Mpeg1: Kaede) in a tank with a net added to induce the adult females to produce eggs after the light turns on, then separate adults from the produced eggs.
  2. Collect the embryos the next day and discard the non-transparent ones which are not viable. Keep approximately 60 embryos per Petri dish (100 mm in diameter) in E3 medium37 and incubate at 28 °C. Remove dead and abnormal embryos, and refresh the E3 medium daily.

3. Preparation of Injection Needles

  1. Prepare the glass microcapillary needles for injection using a micropipette puller instrument. Use the following settings: heat: 772, pull: 100, vel: 200, time: 40, gas: 75.
  2. Break the needle tip with forceps at the position where the needle has an outer diameter of approximately 20 µm (for 10 µm microspheres), using a light microscope with a scale bar in the ocular. Avoid needles with a very large opening size, as they will compromise survival of the embryos.
    NOTE: The opening may be chosen to be smaller or larger, depending on the size and shape of biomaterials to be injected. In the literature, injections using needles with an opening of approximately 50 µm have been reported to cause a significant decrease in embryo survival38.

4. Injection of "Bacteria-Only" or Bacteria-microspheres Suspension into Zebrafish Embryos

  1. Heat agarose solution (1–1.5% (wt) in demi-water) using a microwave oven and pour into a 100-mm Petri dish. Place a plastic mold template on top of the agarose solution in the Petri dish to create indentations in the agarose for placing embryos in proper positions, facilitating injections. Incubate at room temperature and remove the mold when the agarose solution has solidified.
  2. At 3 d post-fertilization, place the embryos in a 100 mm Petri dish containing 0.02% (w/v) 3-aminobenzoic acid (Tricaine) to anaesthetize them. After 5 min, transfer the embryos to the agarose plate overlaid with E3 medium containing 0.02% (w/v) Tricaine and align them in one orientation for injection. For the Mpeg1: Kaede transgenic line first anaesthetize embryos in E3 medium containing 0.02% (w/v) tricaine. Then select embryos expressing green fluorescent proteins using a stereo fluorescence microscope.
  3. Load the needle with approximately 10 µL of the "Bacteria-only" or Bacteria-Microspheres suspension using a microloader pipette tip. Mount the needle onto a micromanipulator connected to the micro-injector. For the injector used here (see Table of Materials), use the following settings for injections of 2–3 nL: pressure: 300–350, back pressure: 0, time: 2 ms.
    NOTE: The settings for the micro-injector depend on the injector used. Injector settings may need to be adjusted for injections of bacteria mixed with biomaterials with other shapes or sizes.
    1. Use needles with the same opening for the injection of the "Bacteria-only" suspension and the Bacteria-Microspheres suspension. If the needle is broken or clogged, always change for a new needle for further injections.
  4. Insert the needle into the muscle tissue of embryos under a light microscope (Figure 1), at an angle of 45–60° between the needle and the body of embryos. Adjust the position of the needle in the tissue by gently moving it back and forth. Inject the embryos using a foot pedal connected to the micro-injector.
  5. After injection of fluorescent bacteria, score the embryos for successful infection under a stereo fluorescence microscope. Discard the embryos scored negative (no visible fluorescent bacteria or no visible fluorescent microspheres). Maintain embryos individually in E3 medium in 48-well plates. Refresh the medium daily.

5. Crushing of Embryos, Microscopic Scoring, and Quantitative Culture of Bacteria

  1. Score all embryos microscopically for the presence of fluorescent bacteria using a stereo fluorescence microscope, starting immediately after the injections, and on each subsequent day until the embryos are randomly selected for quantitative culture.
  2. Randomly select a few live infected embryos (5 to 6 in the present study) shortly after injection and transfer them individually to separate 2 mL microtubes using sterile tips. Remove the medium, wash the embryos gently with sterile PBS once and add 100 µL of sterile PBS.
  3. Add 2–3 sterile zirconia beads (2 mm in diameter) to each vial and crush the embryos using the homogenizer (see Table of Materials) at 3,500 rpm for 30 s. Culture the homogenate quantitatively as described in step 1.3.
    NOTE: Other homogenizers may require different settings.
  4. Randomly select multiple embryos on subsequent days after injection for quantitative culture according to step 5.3.

6. Fluorescence Microscopy of Infection Progression and Provoked Cell Infiltration in Zebrafish Embryos

  1. Anaesthetize the embryos as described in step 4.2. Pipette 500 µL of a PBS-2% (wt) methyl cellulose solution into a Petri dish containing E3 medium with 0.02% (w/v) Tricaine. Place the embryos in the methyl cellulose solution and keep them straight and horizontal.
    NOTE: Methyl cellulose solution is used as a “glue”, which due to its viscosity, can temporarily immobilize embryos in best orientation for imaging.
  2. Use a stereo fluorescence microscope equipped with bright field, mCherry, green fluorescent protein (GFP), and UV filters to image individual embryos under identical optimized settings (e.g., intensity, gain, and exposure time) at 160x magnification. Set the focal plane such that the tissue damage caused by the injection is in focus, using the bright field filter. Set the Z-stack depth at 10 µm and step size at 5 µm, which allows for recording of 3 consecutive images.
  3. Image individual embryos once daily from 5 h post-injection until 2 days post-injection. Exclude dead embryos (no heartbeat or embryo partly degraded) for further imaging and analysis. Maintain embryos individually in E3 medium in 48-well plates. Refresh the medium daily.

7. Quantitative Analysis of Fluorescence Intensity of Infection Progression and Provoked Cell Infiltration Using Object J Project File “Zebrafish-Immunotest”

  1. Download “Zebrafish-Immunotest” and the detailed manual from the link: <https://sils.fnwi.uva.nl/bcb/objectj/examples/zebrafish/MD/zebrafish-immunotest.htmL>, as described in a previous study33. In brief, open images for analysis with “Zebrafish-Immunotest”, operating under the freeware program Image J. In each loaded image, manually mark the injection site based on the observed tissue damage of embryos.
    NOTE: The marked site is used by “Zebrafish-Immunotest” as the center point to detect the fluorescence peak within a distance of 50 µm. The detected fluorescence peak is then used as the center of a standardized area (diameter of 100 µm) for fluorescence measurement.
  2. Click “calculation” in the Object J menu to run the fluorescent measurement for multiple channels, if applicable, automatically for all images. Export the data and analyze by appropriate statistic test methods.

Subscription Required. Please recommend JoVE to your librarian.

Representative Results

The present study assessed the applicability of zebrafish embryos as a novel vertebrate animal model for investigating biomaterial-associated infection. Microinjection technique has been commonly used to inject different bacterial species into zebrafish embryos to cause infection22,26,27,30,36. Using the procedure depicted in Figure 1, S. aureus alone or together with 10 µm PS microspheres (PS10) were injected into the muscle tissue of zebrafish embryos in the present study. Intramuscular injection of S. aureus caused dose-dependent infection in embryos (Figure 2). The doses injected were close to the aimed challenge doses (Day 0 in Figure 2). Only minor variations within groups were observed. Embryos injected with high challenge doses showed variable infection progression at 1 day and 2 days post-injection (Figure 2, 6000 and 2000 CFU). The injected S. aureus bacteria either were eradicated or had proliferated and subsequently established high levels of infection within the embryos. This is similar to the reported progression of S. aureus infection after intravenous injection into zebrafish embryos26. Embryos injected with low challenge doses of S. aureus cleared the bacteria (Figure 2, 600 and 200 CFU). These results indicated that the challenge dose of S. aureus strongly influences their infection progression in zebrafish embryos.

Co-injection of bacteria and microspheres resulted in higher numbers of bacteria injected than injection of bacteria only (data not shown). By preparing the bacterial inoculum for the "Bacteria-only" injections at a higher concentration (approximately 1.5 times higher) than in the Bacteria-Microspheres suspension, we were able to overcome the difference in numbers of CFU injected. This way, it is possible to inject similar numbers of bacteria into embryos in the presence and in the absence of PS10 (day 0, Figure 3). The numbers of microspheres per injection varied. As an example, in one of our experiments, half of the embryos received 1 to 2 microspheres per injection (12 out of 25 embryos in the S. aureus + PS10 group), some received 3 to 4 (8 out of 25 embryos), and a few received 5 to 7 microspheres (5 out of 25 embryos). However, such variations did not influence the levels of the provoked cellular responses, as reported in a previous study33.

Next, we investigated whether the presence of microspheres has an impact on the infection progression in zebrafish embryos challenged with low doses of S. aureus. To this end, we injected approximately 600 CFU of S. aureus-mCherry with or without PS10. We used two methods to study the infection progression: (i) conventional quantitative culture of the infected embryos after crushing, and (ii) scoring of microscopic detection ("microscopic scoring") of fluorescent bacteria (S. aureus-mCherry). We compared the results from these two methods. The score was defined as "yes or no" visibility of fluorescent bacteria in the embryos, regardless of the fluorescence intensity. Our results showed that all embryos with more than 20 CFU of S. aureus-mCherry were positive in microscopic scoring (red dots in Figure 3). For 600 CFU of S. aureus per embryo, the presence of PS10 seemed not to significantly influence the infection progression. At all the time points, both the frequency of infected embryos (indicated on top of Figure 3, low challenge dose) and the numbers of CFU after crushing were not different for embryos with or without PS10 (Figure 3, low challenge dose). This suggested that higher challenge doses of S. aureus are required for studying the potential effects of biomaterials on infection progression in zebrafish embryos. Hence, we injected approximately 1,000 CFU of S. aureus in the presence and absence of PS10 into embryos. The microscopic scoring did not show differences in frequency of the infected embryos with and without PS10 at any time point (Figure 3, high challenge dose). The quantitative culture, however, showed higher CFU numbers retrieved from embryos in the S. aureus + PS10 group than those retrieved from the S. aureus-only group at 2 days post-injection (Figure 3, high challenge dose).

To quantify the extent of infection in the presence and in the absence of biomaterials in zebrafish embryos by image analysis, we recorded a series of images showing the infection progression of S. aureus-mCherry (1,000 CFU per embryo) in the presence and absence of PS10 in live embryos over time (Figure 4A). We also recorded the provoked infiltration of Kaede green fluorescent protein-expressing macrophages in the embryos to quantify the immune cell response (Figure 4B). Kaede fluorescent protein may undergo color conversion from green to red under exposure to UV light, depending on the exposure time and light intensity39. However, such color conversion was not observed under the experimental condition used in the present study. The fluorescence intensity of the infecting bacteria as well as of the infiltrating macrophages within a standardized area around the injection site was measured by our ObjectJ project file "Zebrafish-Immunotest", operating within Image J. "Zebrafish-Immunotest" defines a standardized area with a diameter of 100 µm (yellow circles in Figure 4) around an indicated point of injection. In the embryos, this area included the majority of the fluorescent bacteria residing in the proximity of the injected microspheres, as well as the infiltrating macrophages. The presence of a biomaterial was shown to influence both initial susceptibility to infection and immune cell responses. At 5 h post-injection, macrophage infiltration in response to S. aureus only was significantly higher than in response to S. aureus + PS10 (Figure 5, macrophage infiltration, 5 hpi). At 1 day post-injection embryos with PS10 showed significantly higher levels of S. aureus infection than embryos without PS10 (Figure 5, infection progression, 1 dpi). Thus, these quantitative results demonstrated that the combination of fluorescence image recording and the ObjectJ project file "Zebrafish-Immunotest" can be used to quantify the infection progression and provoked immune cell response in the presence of a biomaterial in the zebrafish embryo model. The model allows for assessing small differences in immune cell responses and levels of bacterial infection in vivo, and it only requires a stereo fluorescence microscope (with image recording) and the open-access "Zebrafish-Immunotest" for evaluation.

Figure 1
Figure 1: Schematic procedure of co-injection of Bacteria-Microspheres suspension into the tail muscle of zebrafish embryos. This figure has been modified from Zhang et al.33 with permission. Please click here to view a larger version of this figure.

Figure 2
Figure 2: Numbers of CFU of S. aureus retrieved from zebrafish embryos injected with inocula, ranging from 6,000 to 200 CFU per embryo and assessed at 0 to 2 days post-injection. The red lines represent the median numbers of CFU. Please click here to view a larger version of this figure.

Figure 3
Figure 3: Numbers of CFU and microscopic scoring of mCherry protein-expressing S. aureus (S. aureus-mCherry) in zebrafish embryos, assessed at different time points. Low challenge dose: 600 CFU per embryo; High challenge dose: 1,000 CFU per embryo; PS10: 10 µm PS microspheres; "+", embryos injected with S. aureus-mCherry together with PS10; "-", embryos injected with S. aureus-mCherry only, so without PS10. Embryos were microscopically scored for fluorescent bacteria and randomly selected for quantitative culture of bacteria after crushing of embryos at the day of injection (Day 0) and at Day 1 and Day 2 post-injection. The embryos microscopically scored positive and negative for fluorescent bacteria are shown in red and black dots, respectively. The numbers of microscopically positive-scoring embryos divided by the total numbers of embryos scored (frequency of infected embryos) at each time point are indicated at the top of the graph. Differences in frequencies of infected embryos and in numbers of CFU between the S. aureus + PS10 and S. aureus only groups at each time point were analyzed by the Fisher' exact test and Mann-Whitney test, respectively. *≤ 0.05. Please click here to view a larger version of this figure.

Figure 4
Figure 4: Representative images recording the infection progression of mCherry-expressing S. aureus (A, red) in the presence and absence of 10 µm PS microspheres (PS10, blue) and the provoked infiltration of Kaede protein-expressing macrophages (B, green) in embryos, from 5 h post-injection (hpi) to 2 days post-injection (dpi). Non-treated embryos (NT) were used as controls. The yellow circles (100 µm in diameter) indicate the standardized area at the injection site for fluorescence quantification using the ObjectJ project file "Zebrafish-Immunotest'. The quantified fluorescence of bacteria and of macrophages is depicted in Figure 5. Scale bars = 100 µm. Please click here to view a larger version of this figure.

Figure 5
Figure 5: Fluorescence quantification of S. aureus infection progression and the provoked macrophage infiltration in the presence and absence of 10 µm PS microspheres (PS10) in zebrafish embryos from 5 hours post-injection (hpi) to 2 days post-injection (dpi), using the ObjectJ project file "Zebrafish-Immunotest". A standardized area at the injection site was used for fluorescence quantification (with a diameter of 100 µm, indicated as the yellow circles in Figure 4). Non-treated embryos (NT) were used as controls. Differences between each two groups at each time point were analyzed by the Mann-Whitney test, *p ≤ 0.05, **p < 0.01, ***p < 0.001. Please click here to view a larger version of this figure.

Subscription Required. Please recommend JoVE to your librarian.


Biomaterial-associated infection (BAI) is a serious clinical complication. A better understanding of the pathogenesis of BAI in vivo would provide new insights to improve the prevention and treatment of BAI. However, current experimental BAI animal models such as murine models are costly, labor-intensive, and require specialized personnel trained in complex surgical techniques. Therefore, these models are not suitable for high throughput analysis. Since requirements for zebrafish embryo models are less complex and costs in general are lower than for murine models, the present study assessed whether zebrafish embryos can be used as a novel vertebrate animal model for investigating BAI in vivo, complementary to the mammalian models.

In order to set up the zebrafish embryo BAI model, we developed a protocol of co-injection of bacteria and microspheres based on a method for intramuscular injection of microspheres into embryos described before33. In this way, most of the bacteria are present in the vicinity of the microspheres in embryos, mimicking the bacteria-biomaterial interaction that takes place during or shortly after the implantation of biomaterials in humans/mammals.

To be able to compare infection progression in the presence and in the absence of microspheres in zebrafish embryos, embryos should be challenged with similar initial numbers of bacteria with and without microspheres. However, according to our experience, co-injection of Bacteria-Microspheres suspension results in more bacteria being injected than injection of "Bacteria-only" suspension. To address this issue, the ratio between the concentration of bacteria in "Bacteria-only" suspensions (without microspheres) and in Bacteria-microspheres suspensions should be tailored. In the present study, the concentration of S. aureus in the "Bacteria-only" suspension needed to be approximately 1.5 times higher than the concentration in the Bacteria-Microspheres suspension. Whether this ratio also applies to other bacterial species and other biomaterials remains to be tested. Of note, to inject similar numbers of bacteria with and without microspheres, the opening of the needles used for injections of either suspension should be as close to identical as possible.

Several properties of a biomaterial such as shape and size play an important role in determining its injectability and co-injection with bacteria. In the present study, we used 10 µm polystyrene microspheres (PS10) as model biomaterials. According to our experience, microspheres of a size of up to 15 µm are injectable for 3 days old embryos following the protocol developed in the present study33. For microspheres of a relatively large size (e.g., ≥ 10 µm), we discourage the use of non-monodispersed or irregularly shaped microspheres/microparticles which tend to cause clogging of the needle. If biomaterials in other shapes than round and in different sizes are chosen to be used, their injectability needs to be tested. For (co-)injection of microspheres and bacteria, we used a 4% polyvinylpyrrolidone (PVP) solution to facilitate dispersion. This may be helpful for injection of biomaterials with and without bacteria into embryos in general.

As was the case for injections of microspheres only33,40, the numbers of microspheres injected together with bacteria into embryos varied per injection, mostly ranging from 1 to 4 microspheres per embryo. However, since such variations did not result in differences in levels of the provoked immune cell response in embryos33, they were also not expected to influence the potential effects of microspheres on infection progression. Nevertheless, novel approaches allowing injections of a single microsphere (alone or together with bacteria) would be desired.

We assessed whether microscopic scoring of presence of fluorescent bacteria can be used as a "yes or no" scoring system to analyze infection progression in live embryos. The criterion of a positive microscopic score was defined as the presence of visible fluorescent bacteria, regardless of the fluorescence intensity. Compared to quantitative culture of bacteria, our representative results suggested that microscopic scoring can distinguish embryos with 20 or more CFU of S. aureus bacteria from embryos with lower numbers of CFU or no infection. Thus, since only low numbers of bacteria are required for a positive score, this method is almost as sensitive as quantitative culture. Since the embryos do not need to be sacrificed and no high-end microscopes or sorting systems for fluorescence are required to perform analyses using this method, we consider microscopic scoring a simple but reliable method to monitor the infection progression of bacteria in live embryos. For quantitative analysis of the level of infection (rather than the "yes or no" scoring system as described above) and immune cell response in single live embryos, we applied the ObjectJ project file "Zebrafish-Immunotest" to quantify fluorescence intensity of the fluorescent bacteria and fluorescent macrophages recorded over time. We used a standardized area (with a diameter of 100 m) surrounding the injection site to measure fluorescence, since this area was shown to include a majority of the bacteria and the infiltrating macrophages. A detailed manual of "Zebrafish-Immunotest" was published previously33,40. Of note, "Zebrafish-Immunotest" is an open access plug-in for ImageJ, which can be tailored by the user. For instance, the diameter of the area of analysis and other parameters of "Zebrafish-Immunotest" can be freely changed according to the study setup (see examples in the link provided in step 7 in the Protocol).

In order to show the possible infection-enhancing effects of biomaterials in zebrafish embryos, the challenge dose of bacteria needs to be assessed. In the present study, we found that a challenge dose of 1,000 CFU of S. aureus per embryo or higher is required. Higher levels of S. aureus infection in embryos with PS10 than in those without PS10 were found on the first 2 days after injection, indicating that the presence of biomaterials transiently facilitates outgrowth of S. aureus in the embryos. Whether infection remains at high levels in presence of biomaterials at later time points should be studied using older embryos under ethical approval according to applicable regulations. Since the clearance of S. aureus in zebrafish embryos is mainly dependent on phagocytosis and killing by macrophages and neutrophils23,24, the outgrowth of bacteria might be explained by a reduced effectiveness of the phagocytes to kill the bacteria due to the presence of biomaterials. This is in line with the well-known infection-risk enhancement by biomaterials in patients2,4,15, also commonly observed in more complex animal models such as mouse and other animal models10,11,12,13. In addition to S. aureus infection, infection progression of S. epidermidis or other pathogens in the presence of biomaterials can be investigated following the protocol described in the present study. From the point of biomaterials, several material properties (e.g., chemical composition, hydrophobicity, roughness, and surface charges) may influence the cellular responses and/or bacteria-material interaction41,42. Our previous study has shown that injection of a biomaterial (in the presence of PVP) provoked a stronger macrophage infiltration compared to injection of only PVP in zebrafish embryos. Moreover, zebrafish embryos reacted differently to microspheres made of poly (-caprolactone) and polystyrene33. Therefore, injection of microspheres of different nature may also have differential effects on enhancement of infection, which can be relatively easily assessed by the method described here.

For further development, this zebrafish embryo BAI model may be amended for a high throughput system featuring automated robotic injection27,43, complex object parametric analysis and sorting (COPAS) systems, and high throughput RNA sequence analysis27,44. Such zebrafish embryo-based high throughput BAI models may be used as whole animal systems for in vivo screening and testing of (novel) anti-infective biomaterials as well as testing of the efficacy of antibiotic treatments or other anti-BAI strategies. Moreover, intracellular survival is one major strategy of bacteria to survive in the presence of biomaterials9,10,11,12,13. The usefulness of zebrafish embryos for studying intracellular infection has been shown in several studies36,46. Thus, our embryo model may be used to study the intracellular survival of staphylococci or other intracellular pathogens in the presence of biomaterials, and strategies to treat such intracellular infections. In addition, in situ hybridization techniques45 can be used in the model to study the influence of bacteria or biomaterials or their combination on the expression of particular genes at the injection site, which may be helpful to discover marker genes for BAI.

In summary, the present study shows the potential of zebrafish embryos with the methods developed here to study biomaterial-associated infection in real time in vivo. This zebrafish embryo model may therefore be used to investigate novel infection-resistant biomaterials and promising prevention and treatment strategies of BAI, and to close the gap between in vitro studies and larger animal models.

Subscription Required. Please recommend JoVE to your librarian.


The authors have nothing to disclose.


This study was financially supported by the IBIZA project of the BioMedical Material (BMM) program and co-funded by the Dutch Ministry of Economic Affairs. The authors would like to thank Prof. Dr. Graham Lieschke from Monash University, Australia for providing the zebrafish transgenic line (mpeg1:Gal4/UAS:Kaede).


Name Company Catalog Number Comments
Tryptic soya agar BD Difco 236950 Media preparation unit at AMC
Tryptic soya broth BD Difco 211825
Polyvinylpyrrolidone40 Applichem A2259.0250
10 µm diameter polystyrene microspheres (blue fluorescent) Life technology/ThemoFisher F8829
Glass microcapilary (1 mm O.D. x 0.78 mm I.D.) Harvard Apparatus 30-0038
Micropipette puller instrument Sutter Instrument Inc Flaming p-97
Light microscope LM 20 Leica MDG33 10450123
3-aminobenzoic acid (Tricaine) Sigma-Aldrich E10521-50G
Agarose MP Roche 11388991001
Stereo fluorescent microscope LM80 Leica MDG3610450126
Microloader pipette tips Eppendorf 5242956.003
Micromanipulator M3301 with M10 stand World Precision Instruments 00-42-101-0000
FemtoJet express micro-injector Eppendorf 5248ZO100329
Microtrube 2 mL pp Sarstedt 72.693.005
Zirconia beads Bio-connect 11079124ZX
MagNA lyser Roche 41416401
MSA-2 plates (Mannitol Salt Agar-2) Biomerieux 43671 Chapmon 2 medium
Methyl cellulose 4000cp Sigma-Aldrich MO512-250G
Chloramphenicol Sigma-Aldrich C0378
Gyrotory shaker (for bacterial growth) New Brunswick Scientific G10
Zebrafish incubator VWR Incu-line
Cuvettes BRAND 759015
Centrifuge Hettich-Zentrifugen ROTANTA 460R
Spectrometer Pharmacia biotech Ultrospec®2000
Forceps Sigma-Aldrich F6521-1EA
48 well-plates Greiner bio-one 677180
96 well-plates Greiner bio-one 655161
Petri dish Falcon 353003
Petri dish Biomerieux NL-132
ImageJ Not applicable Not applicable link: https://imagej.nih.gov/ij/download.html
GraphPad 7.0 Prism Not applicable



  1. Williams, D. F. On the nature of biomaterials. Biomaterials. 30, 5897-5909 (2009).
  2. Busscher, H. J., et al. Biomaterial-Associated Infection: Locating the Finish Line in the Race for the Surface. Science Translational Medicine. 4, 153rv10 (2012).
  3. Otto, M. Staphylococcus epidermidis - the 'accidental' pathogen. Nature Reviews Microbiology. 7, 555-567 (2009).
  4. Moriarty, T. F., et al. Orthopaedic device-related infection: current and future interventions for improved prevention and treatment. EFORT Open Reviews. 1, 89-99 (2016).
  5. Campoccia, D., Montanaro, L., Arciola, C. R. The significance of infection related to orthopedic devices and issues of antibiotic resistance. Biomaterials. 27, 2331-2339 (2006).
  6. Schierholz, J. M., Beuth, J. Implant infections: a haven for opportunistic bacteria. Journal of Hospital Infection. 49, 87-93 (2001).
  7. Zimmerli, W., Lew, P. D., Waldvogel, F. A. Pathogenesis of foreign body infection. Evidence for a local granulocyte defect. Journal of Clinical Investigation. 73, (4), 1191-1200 (1984).
  8. Boelens, J. J., et al. Biomaterial-associated persistence of Streptococcus epidermidis in pericatheter macrophages. Journal of Infectious Diseases. 181, (4), 1337-1349 (2000).
  9. Broekhuizen, C. A. N., et al. Tissue around catheters is a niche for bacteria associated with medical device infection. Critical Care Medicine. 36, 2395-2402 (2008).
  10. Riool, M., et al. Staphylococcus epidermidis originating from titanium implants infects surrounding tissue and immune cells. Acta Biomaterial. 10, 5202-5212 (2014).
  11. Zaat, S. A. J., Broekhuizen, C. A. N., Riool, M. Host tissue as a niche for biomaterial-associated infection. Future Microbiology. 5, 1149-1151 (2010).
  12. Broekhuizen, C. A. N., et al. Staphylococcus epidermidis is cleared from biomaterial implants but persists in peri-implant tissue in mice despite rifampicin/vancomycin treatment. Journal of Biomedical Materials Research Part A. 85, 498-505 (2008).
  13. Broekhuizen, C. A. N., et al. Peri-implant tissue is an important niche for Staphylococcus epidermidis in experimental biomaterial-associated infection in mice. Infection and Immunity. 75, 1129-1136 (2007).
  14. Zimmerli, W., Sendi, P. Pathogenesis of implant-associated infection: the role of the host. Seminars in Immunopathology. 33, 295-306 (2011).
  15. Darouiche, R. O. Current concepts - Treatment of infections associated with surgical implants. New England Journal of Medicine. 350, 1422-1429 (2004).
  16. Riool, M., de Breij, A., Drijfhout, J. W., Nibbering, P. H., Zaat, S. A. J. Antimicrobial peptides in biomedical device manufacturing. Frontiers in Chemistry. 5, 63 (2017).
  17. Brooks, B. D., Brooks, A. E., Grainger, D. W. Antimicrobial medical devices in preclinical development and clinical use. Biomaterials Associated Infection. Moriaty, F. T., Zaat, S. A., Busscher, H. J. Springer. New York, NY, USA. 307-354 (2013).
  18. Sjollema, J., et al. The potential for bio-optical imaging of biomaterial-associated infection in vivo. Biomaterials. 31, 1984-1995 (2010).
  19. Suri, S., et al. In vivo fluorescence imaging of biomaterial-associated inflammation and infection in a minimally invasive manner. Journal of Biomedical Materials Research Part A. 103, 76-83 (2015).
  20. Zhou, J., Hu, W. J., Tang, L. P. Non-invasive characterization of immune responses to biomedical implants. Annals of Biomedical Engineering. 44, 693-704 (2016).
  21. van Oosten, M., et al. Real-time in vivo imaging of invasive- and biomaterial-associated bacterial infections using fluorescently labelled vancomycin. Nature Communications. 4, 2584 (2013).
  22. Lesley, R., Ramakrishnan, L. Insights into early mycobacterial pathogenesis from the zebrafish. Current Opinion in Microbiology. 11, 277-283 (2008).
  23. Brannon, M. K., et al. Pseudomonas aeruginosa Type III secretion system interacts with phagocytes to modulate systemic infection of zebrafish embryos. Cellular Microbiology. 11, 755-768 (2009).
  24. Wiles, T. J., Bower, J. M., Redd, M. J., Mulvey, M. A. Use of zebrafish to probe the divergent virulence potentials and toxin requirements of extraintestinal pathogenic Escherichia coli. PLoS Pathogens. 5, e1000697 (2009).
  25. Prajsnar, T. K., et al. Zebrafish as a novel vertebrate model to dissect enterococcal pathogenesis. Infection and Immunity. 81, 4271-4279 (2013).
  26. Prajsnar, T. K., Cunliffe, V. T., Foster, S. J., Renshaw, S. A. A novel vertebrate model of Staphylococcus aureus infection reveals phagocyte-dependent resistance of zebrafish to non-host specialized pathogens. Cellular Microbiology. 10, 2312-2325 (2008).
  27. Veneman, W. J., et al. A zebrafish high throughput screening system used for Staphylococcus epidermidis infection marker discovery. BMC Genomics. 14, 255 (2013).
  28. Renshaw, S. A., Trede, N. S. A model 450 million years in the making: zebrafish and vertebrate immunity. Disease Model and Mechanism. 5, 38-47 (2012).
  29. Meijer, A. H., van der Vaart, M., Spaink, H. P. Real-time imaging and genetic dissection of host-microbe interactions in zebrafish. Cellular Microbiology. 16, 39-49 (2014).
  30. Spaink, H. P., et al. Robotic injection of zebrafish embryos for high-throughput screening in disease models. Methods. 62, 246-254 (2013).
  31. Riool, M., et al. A chlorhexidine-releasing epoxy-based coating on titanium implants prevents Staphylococcus aureus experimental biomaterial-associated infection. European Cells and Materials. 33, 143-157 (2017).
  32. Ellett, F., Pase, L., Hayman, J. W., Andrianopoulos, A., Lieschke, G. J. Mpeg1 promoter transgenes direct macrophage-lineage expression in zebrafish. Blood. 117, E49-E56 (2011).
  33. Zhang, X., et al. The zebrafish embryo as a model to quantify early inflammatory cell responses to biomaterials. Journal of Biomedical Materials Research Part A. 105, 2522-2532 (2017).
  34. Traber, K., Novick, R. A slipped-mispairing mutation in AgrA of laboratory strains and clinical isolates results in delayed activation of agr and failure to translate delta- and alpha-haemolysins. Molecular Microbiology. 59, 1519-1530 (2006).
  35. Rosen, J. N., Sweeney, M. F., Mably, J. D. Microinjection of zebrafish embryos to analyze gene function. Journal of Visualized Experiments. (25), e1115 (2009).
  36. Benard, E. L., et al. Infection of zebrafish embryos with intracellular bacterial pathogens. Journal of Visualized Experiments. 61, 3781 (2012).
  37. Brand, M., Granato, M., Christiane, N. -V. Keeping and raising zebrafish. Zebrafish, A Practical Approach. Dahm, R., Nüsslein-Volhard, C. Oxford University press. Oxford, UK. 7-37 (2002).
  38. Chaplin, W. T. P. Development of a microinjection platform for the examination of host-biomaterial interactions in zebrafish embryos. Queen's University. Master thesis (2017).
  39. Ando, R., Hama, H., Yamamoto-Hino, M., Mizuno, H., Miyawaki, A. An optical marker based on the UV-induced green-to-red photoconversion of a fluorescent protein. Proceedings of the National Academy of Science of the United States of America. 99, 12651-12656 (2002).
  40. Witherel, C. E., Gurevich, D., Collin, J. D., Martin, P., Spiller, K. L. Host-biomaterial interactions in zebrafish. ACS Biomaterials Science & Engineering. 4, 1233-1240 (2018).
  41. Anderson, J. M. Biological responses to materials. Annual Review of Materials Research. 31, 81-110 (2001).
  42. Onuki, Y., Bhardwaj, U., Papadimitrakopoulos, F., Burgess, D. J. A review of the biocompatibility of implantable devices: current challenges to overcome foreign body response. Journal of Diabetes Science and Technology. 2, 1003-1015 (2008).
  43. Carvalho, R., et al. A High-Throughput Screen for Tuberculosis Progression. PLoS One. 6, e16779 (2011).
  44. Stockhammer, O. W., et al. Transcriptome analysis of Traf6 function in the innate immune response of zebrafish embryos. Molecular Immunology. 48, 179-190 (2010).
  45. Thisse, C., Thisse, B. High-resolution in situ hybridization to whole-mount zebrafish embryos. Nature Protocols. 3, 59 (2007).
  46. Prajsnar, T. K., et al. A privileged intraphagocyte niche is responsible for disseminated infection of Staphylococcus aureus in a zebrafish model. Cellular Microbiology. 14, 1600-1619 (2012).



    Post a Question / Comment / Request

    You must be signed in to post a comment. Please or create an account.

    Usage Statistics