TB, AK, JF, and DN received grant support for the Strategic Research Centre (SRC) &#34;An evidence-based preclinical framework for the development of antimicrobial therapeutics in cystic fibrosis&#34; (PIPE-CF; Project No. SRC 022) from the UK Cystic Fibrosis Trust and US Cystic Fibrosis Foundation. LD and JF acknowledge funding from Kidney Research North West (Project No. 49/19).

In this study, Galleria mellonella (greater wax moth) larvae were selected as a model for antibiotic susceptibility testing and acute toxicity trials. No ethical approval is required for the experimental use of Galleria mellonella. The details of the reagents and equipment used are listed in the Table of Materials.
1. Experimental design
<ol>
	<li>Determine the appropriate Galleria mellonella larvae group sizes based on the proportional change in larval survival that the study aims to capture. Table 1 details the group sizes required to detect specific percentage changes in survival using a Pseudomonas aeruginosa strain PAO1 infection model. 
	NOTE: When using a novel pathogen, first determine inter-assay variability in the proportional survival of infected but untreated larvae, as this will influence sample size determination.
	<ol>
		<li>Include two groups of PBS controls: one injected before the rest of the infections to ensure the syringe is sharp and fit for use, and another injected during or after bacterial infections to ensure proper sterilization between infection groups. If optimizing with a new pathogen, include a heat-treated control to ensure that death is not the result of an immune response to foreign particles. 
		NOTE: Insulin syringes could be used for injections, reducing the risks of blunting and contamination. However, experiments may routinely use hundreds of G. mellonella, making the use of insulin syringes costly and wasteful.</li>
		<li>For studies optimizing antibacterial treatment, include two additional controls: a group infected with bacteria and then injected with a vehicle &#39;sham&#39; treatment, and a group injected twice with the vehicle, once at the time of infection for the other conditions and once at the time of treatment. 
		NOTE: The former is an untreated control, while the latter controls for any trauma caused by the injections. Such trauma is more likely when blunt needles are used.</li>
	</ol>
	</li>
	<li>Order G. mellonella from a live bait supplier, or maintain a colony of G. mellonella as previously described5,6,7. For the supplier listed in the Table of Materials, order 1.8 times the planned number of larvae, as approximately 33% will be excluded based on size, and a further 10% may die following cuticle sterilization.
	<ol>
		<li>Determine G. mellonella weight variability prior to experimental use, and ensure that the weight range does not exceed one standard deviation of the mean. 
		NOTE: For suppliers not listed in the Table of Materials, arrange for the supplier to provide new stock.</li>
	</ol>
	</li>
	<li>Upon receipt, store G. mellonella at room temperature to limit the chance of cocooning, which occurs following incubation at 37 &#176;C. 
	NOTE: Not all larvae from commercial suppliers form cocoons, which have previously been used as an indicator of larval health16.</li>
	<li>Use larvae within 1 week of receipt, in which case they do not require feeding. 
	NOTE: Although the larval life stage will vary between batches, most larvae are delivered during the last instar before pupating. In this stage, feeding naturally decreases compared to earlier stages17.</li>
</ol>
2. Sterilization and selection of G. mellonella larvae
<ol>
	<li>Weigh Galleria mellonella larvae and discard any that fall outside the range of 224 mg &#177; 49.2 mg, which is the average weight of the larvae plus or minus one standard deviation. This will result in the exclusion of approximately 33% of the larvae. 
	NOTE: Weight variation may differ between suppliers. For suppliers not listed in this protocol, calculate an appropriate weight range.</li>
	<li>Perform the following steps under aseptic conditions.</li>
	<li>Spray 70% ethanol into a Petri dish, ensuring enough to cover the bottom of the dish.</li>
	<li>Sterilize the surface of G. mellonella in batches of 10-20 larvae.
	<ol>
		<li>Place each batch individually in the dish and spray the larvae twice with 70% ethanol.</li>
		<li>Use tweezers to roll the larvae, ensuring full coverage.</li>
		<li>Remove the larvae from the ethanol and place them in a sterile Petri dish. Leave the dish uncovered to allow the larvae to dry. 
		CAUTION: Leaving G. mellonella in ethanol for longer than 15 s will result in high mortality.</li>
	</ol>
	</li>
	<li>Once approximately 90% of the larvae have regained activity after 2 h, separate the recovered larvae into groups of a size that will allow sufficient detection of survival changes according to the power calculations detailed in Table 1.</li>
	<li>Use G. mellonella within 6 h of sterilization.</li>
</ol>
3. Optimizing bacterial inoculum density
<ol>
	<li>Prepare a bacterial infection stock of a known CFU/mL prior to infection. Methods for generating stocks will vary by organism. Here, Pseudomonas aeruginosa was grown to mid-log phase in nutrient broth, aliquoted, and frozen at a density of 6 x 107 CFU/mL.</li>
	<li>Pellet the infection stock by centrifuging at 10,000 x g at room temperature for 5 min, and resuspend in PBS. Serially dilute the bacterial stock tenfold to generate a range of inoculum doses of 101-107 CFU per larva, considering that each larva is injected with 10 &#181;L of inoculum. 
	NOTE: The specific inoculum dose range will differ depending on bacterial virulence, but the proposed range here should be suitable for most pathogenic species. In vitro growth rate determination can help inform the selection of an appropriate dose range, as strain-specific growth rate in liquid culture is correlated with larval mortality.</li>
	<li>Before beginning infections, enumerate the inoculum with a Miles and Misra serial dilution to accurately determine inoculum density18.</li>
	<li>Prepare three 1 mL microfuge tubes containing either sterile dH2O, 70% ethanol, or sterile PBS. These will be used continually to sterilize the syringe used to inject the larvae.</li>
	<li>Inspect a sterile 100 &#181;L Hamilton syringe, ensuring the needle tip is sharp and has not developed a hook, which will cause significant trauma to the infection site. 
	CAUTION: A Hamilton syringe needle tip will begin to warp after approximately 300 infections. If the needle tip is warped, it must be replaced.</li>
	<li>Wash the syringe sequentially with dH2O, ethanol, and PBS prior to infections, drawing up and discarding the maximum capacity of the syringe.</li>
	<li>Vortex the resuspended infection inoculum and draw up a maximum of 100 &#181;L into the Hamilton syringe, sufficient to inject 10 &#181;L per larva.</li>
	<li>Inject each larva with 10 &#181;L of inoculum in the rear right proleg. Ensure that the needle penetrates approximately 2 mm into the body. 
	NOTE: Various methods of infection can be used. These include holding the larva over a pipette tip to expose the prolegs, securing the syringe statically and&#160;positioning the G. mellonella by hand, or injecting freehand.</li>
	<li>Between each set of infections, sterilize the syringe as detailed in step 2.5 to prevent contamination from residual skin commensals.</li>
	<li>Incubate the infected larvae at a temperature sufficient for microbial growth, between 20 &#176;C and 42 &#176;C, which is an appropriate range for G. mellonella survival5.</li>
	<li>Monitor G. mellonella survival at regular intervals from the time at which mortality is usually first observed to accurately measure the time of death. This must be assessed in an initial screen. Remove any dead larvae and record their time of death.</li>
	<li>Select the optimum infection dose for a therapeutic testing study based on the dose that yields 50% mortality by 18 h and over 80% by 72 h. This allows for the development of a rapid single-day screen while ensuring sufficient virulence and an appropriate therapeutic window.</li>
</ol>
4. Toxicity testing of novel antimicrobial agents in uninfected larvae
<ol>
	<li>Assess the toxicity of novel antimicrobials and chosen vehicles in Galleria mellonella prior to their use with experimentally infected larvae. Prepare a broad range of doses exceeding the expected therapeutic range of the antimicrobial, guided by in vitro (e.g., cell line) toxicity data, if available.
	<ol>
		<li>Consider that the larvae will be injected with 10 &#181;L of the therapeutic. Prepare vehicle-only controls at concentrations matching those in which the therapeutic is delivered.</li>
	</ol>
	</li>
	<li>Inject healthy, sterile G. mellonella in appropriate group sizes with the different antimicrobial and PBS vehicle concentrations, as detailed in steps 3.2-3.10. In the present study, the antimicrobial used was tobramycin. 
	NOTE: For agent requiring DMSO as a solvent, inject with a 26s gauge needle, rather than the standard 22 gauge needle, as trauma from larger needles increases mortality when using DMSO.</li>
	<li>Define a safe dose as one that yields no significant difference in mortality compared to larvae injected with PBS only.</li>
</ol>
5. Optimizing treatment of G. mellonella bacterial infection with an antimicrobial agent
<ol>
	<li>Prepare a range of doses of the antimicrobial agent, considering that infected larvae are treated with a 10 &#181;L dose. Use a range of doses with minimal toxicity, as assessed in step 4.</li>
	<li>Follow steps 1 and 2 of this protocol to prepare and infect Galleria mellonella in appropriate groups at the previously optimized infection dose.</li>
	<li>At 2 h post-infection, treat the larvae with the prepared antimicrobial agent or vehicle control solution. Follow steps 3.2-3.8, injecting into the opposite proleg from the one&#160;injected during infection. Sterilize the needle between groups. 
	NOTE: Treatment at 2 h was selected for this optimization to acquire strong dose-response data, from which subsequent optimization of treatment timing was determined19.</li>
	<li>Monitor G. mellonella survival at 30 min intervals or more frequently from the time at which mortality is usually first observed. Remove any dead larvae and record their time of death.</li>
	<li>Calculate the change in survival proportions between the treatment groups. Use Kaplan-Meier survival analysis to determine whether treatment leads to significantly altered larval mortality. Include appropriate post-hoc correction for pairwise multiplicity in multi-group analyses.</li>
</ol>
6. Optimizing treatment timing of infected G. mellonella
<ol>
	<li>Follow steps 1 and 2 to prepare Galleria mellonella in appropriate groups at the previously optimized infection dose.</li>
	<li>Prepare the antimicrobial agent at the dose previously optimized in step 4.</li>
	<li>At either 2 h, 4 h, 6 h, 9 h, or 12 h post-infection, treat the infected larvae following steps 3.2-3.8 to compare how the timing of treatment impacts mortality.</li>
	<li>Monitor G. mellonella survival at 30 min intervals or more frequently from the time at which mortality is usually first observed. Remove any dead larvae and record their time of death. The optimum timing is the one that maintains the survival observed following the initial optimization of the treatment dose. 
	NOTE: When testing antimicrobial efficacy in G. mellonella, optimize both treatment dose and timing separately, using the former to inform the treatment dose in the latter.</li>
</ol>

Standardized Galleria mellonella Models for Preclinical Antimicrobial Testing

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The authors have nothing to disclose.

The burden of antimicrobial resistance (AMR) is continually increasing. In 2019, an estimated 4.95 million deaths were associated with AMR worldwide30. By 2050, the mortality caused by AMR is estimated to reach 10 million31. To address this risk, novel antimicrobials must be developed and tested efficiently and&#160;cost-effectively, necessitating the use of preclinical models that accurately predict antimicrobial efficacy. The high attrition rate observed during translation to clinical trials is a major limiting factor. One study described 13 antibiotic candidates that failed in clinical trials, with 11 failing to progress to phase II32.
The present study provides a framework for the optimization of G. mellonella preclinical antimicrobial screening studies and a method for assessment of antimicrobial efficacy. G. mellonella larvae have considerable utility in evaluating drug toxicity, MIC determination, and virulence testing, while contributing to the reduction of mammals used in preclinical development. Galleria mellonella larvae have relatively high throughput, are biologically relevant, and translate well into more complex mammalian models. Meanwhile, while wild-type laboratory mice cost between &#163;8 and &#163;30 each with ~&#163;7 weekly maintenance per mouse, G. mellonella cost ~&#163;2 for 50 larvae. To test 10 compounds in a G. mellonella model would, therefore, cost ~&#163;60, compared to upwards of &#163;4000 for the same study in mice. Moreover, previous studies have compared the toxicity and efficacy of novel compounds and identified a correlation between acute toxicity in G. mellonella and mice8,19,33. Therefore, implementing a G. mellonella screen to prioritize compounds to be further tested in mouse models is recommended.
Despite the clear utility of the model, there are several considerations to ensure successful application. The lack of research-grade, sterile larvae complicates their preparation for experimental use, as ethanol sterilization is required, or researchers are required to maintain their own G. mellonella colony, which would mitigate the risk of contamination and improve overall experimental quality5,6. Improper sterilization can yield considerable mortality, and it is challenging to entirely sterilize the organism, as longer ethanol exposure time leads to death. Alternative methods of sterilization include swabbing the proleg of each larva with 70% ethanol prior to infection, which would decrease mortality during sterilization, but is a more labor-intensive method. Other antiseptics could also be used, though no alternatives were assessed in this study, as ethanol sterilization yielded &#60;10% death, once optimized. Moreover, it is often unclear whether suppliers treat their G. mellonella with antibiotics, as suppliers may source their larvae from other suppliers rather than maintaining colonies themselves.
G. mellonella biology differs considerably from mammals, which imposes limitations on their utility. Their immune system lacks any adaptive immunity, although key soluble and cellular aspects of innate immunity are present. Hemocytes are a principal innate immune defense of G. mellonella and display phagocyte-like properties. Various subsets of these cells have been described, including granulocytes and plasmatocytes, amongst others34. G. mellonella also cannot recapitulate relevant infection sites, such as those of respiratory or bladder infections. However, in a preclinical pipeline, G. mellonella would serve as a pre-screen to murine models, ensuring that only the most promising compounds would progress through to the complex mammalian system that more closely resembles human infection environments. Finally, the model would benefit from further genomic characterization of G. mellonella to determine its suitability for assessing changes in clinically relevant biomarkers. In particular, this necessitates improving our understanding of G. mellonella immunity.
Overall, the Galleria mellonella infection model is a valuable tool for the preclinical assessment of novel antimicrobial compounds prior to their evaluation in mammalian models. While their usage is complicated by a lack of supply standardization, their application is high throughput, simple, and can be applied broadly across the antimicrobial development landscape. In the future, integration of this model within a standardized preclinical pipeline could accelerate the development of new antimicrobial compounds to increase the proportion of candidates progressing from preclinical evaluation to clinical trials.

Galleria mellonella (the greater wax moth) larvae are used extensively across the biological sciences as infection models for microbial species, and for toxicity testing of novel drug compounds1,2. They have the potential for considerable utility in a preclinical antimicrobial testing pipeline, as they are high throughput, replicate integral in vivo characteristics of human infection, and reduce reliance on mammalian models, in line with the principles of reduction, refinement, and replacement that govern ethical use of mammalian species in research.
Developing new antibiotics requires extensive preclinical testing in vitro and in vivo models prior to clinical validation3. Only a few novel agents with promising preclinical data packages ever translate through to the clinic, and one contributor to this high attrition rate is a failure of preclinical screens to capture the complexities of infection environments4. These issues contribute not only to a low translation rate of antimicrobial agents to the clinic, but also to an increased use of experimental vertebrate animals during late-stage preclinical screening. To improve the preclinical assessment of novel antimicrobials and to reduce the usage of expensive, time-consuming, complex, and ethically problematic murine in vivo models, better early-stage drug screening tools are needed that reduce the number of unpromising compounds progressing through to testing in vertebrate systems.
G. mellonella has a short lifecycle of 8 weeks, comprised of four life stages: egg, larvae, pupae, and adults, of which the larval form is utilized in this protocol1. G. mellonella are easy to maintain throughout an experiment without the requirement for specialist equipment or a dedicated animal research facility. There is no requirement to seek ethical approval for their use, and researchers may breed the organism in-house to improve experimental quality2,5,6,7. The G. mellonella immune system closely resembles that of the mammalian innate immune system, with the ability to respond to &#39;self&#39; and &#39;non-self&#39; stimuli8. Haemocytes are responsible for pathogen-associated molecular pattern recognition and subsequent phagocytosis, playing a role that is functionally analogous to that of neutrophils in humans9. G. mellonella encodes three types of toll-like receptors that have been identified by sequence homology to humans, and produce complement-like proteins, which recognize non-self material and form localized melanization complexes following the activation and polymerization of phenoloxidase into melanin10. This can serve as a visual read-out of larval health during infection experiments, as the cuticle is darkened by melanization. It should be noted, however, that the melanization axis in insects, which involves phenoloxidase, differs substantially from the tyrosinase-melanin axis in mammals11,12. Additionally, G. mellonella produces 18 inducible antimicrobial peptides, including lysozyme and defensin homologues13. This similarity, as well as the straightforward larval maintenance procedures and high throughput nature of the model, have made G. mellonella a widely utilized organism in the assessment of novel drugs. In preclinical antibiotic development, G. mellonella has increased utility compared to in vitro models, as they can more accurately model host-pathogen-drug interactions in a complex environment with active immunity.
At present, there is no standardized research-grade supplier of G. mellonella in Europe. Researchers must instead purchase G. mellonella larvae from bait shops or maintain their own colony. Whilst methods for maintaining an in-house G. mellonella colony have been described and can increase experimental consistency5,6,7, this option is likely to be attractive only to those who use the larvae frequently. As such, this protocol focuses on the experimental setup following the purchase of larvae from a live bait supplier. While more accessible, this method increases experimental complexity and can introduce additional variability into assays due to inconsistencies in the health of the larvae at the point at which they are received from suppliers. For academics, industry, and regulators to accept and adopt G. mellonella testing as part of a preclinical antimicrobial development pipeline, a standardized system for optimization and assessment of antimicrobial efficacy is necessary.
This study optimizes the experimental design of a G. mellonella infection model for antibiotic development. While G. mellonella infection models have been described14,15, the present methodology documents additional steps to mitigate the additional complexity introduced by the inconsistency of supply and provides a framework for the assessment of novel antimicrobials. As a test case, G. mellonella was infected with the WHO priority one pathogen Pseudomonas aeruginosa, and treatment with an aminoglycoside agent (tobramycin) was optimized. This framework, illustrated in Figure 1, provides a foundation for future preclinical antimicrobial screening studies with novel agents.

<table border="1" fo:keep-together.within-page="1" fo:keep-with-next.within-page="always">
	<tbody>
		<tr>
			<td>22s gauge, Small Hub RN Needle, 2 in, point style 2</td>
			<td>Hamilton</td>
			<td>7758-03</td>
			<td>Replacement for the Hamilton syringe.</td>
		</tr>
		<tr>
			<td>Bacterial infection stocks</td>
			<td></td>
			<td></td>
			<td>Bacterial stocks of a known density (CFU/mL) frozen during mid-exponential phase of growth.&#160;</td>
		</tr>
		<tr>
			<td>Ethanol</td>
			<td>Fisher Scientific</td>
			<td>10610813</td>
			<td>Other manufacturers may be used.</td>
		</tr>
		<tr>
			<td>G. mellonella larvae</td>
			<td>Livefoods</td>
			<td>5.06045E+12</td>
			<td>For this supplier, orders are marked as &#8220;New stock for lab use&#8221;. As of April 2024, new stock is delivered to the supplier on Mondays. Orders should be placed then, for delivery on Wednesdays.</td>
		</tr>
		<tr>
			<td>Microliter syringe</td>
			<td>Hamilton</td>
			<td>80630</td>
			<td>The 80630 syringe has a 100 &#181;L capacity. Other volumes exist, such as the 80430, 80530 or 80730.</td>
		</tr>
		<tr>
			<td>Petri dish</td>
			<td>Fisher Scientific</td>
			<td>12674785</td>
			<td>Other manufacturers may be used.</td>
		</tr>
	</tbody>
</table>

galleria mellonella as an antimicrobial screening model

To combat the rising global issue of antibiotic resistance, the accelerated development of novel antibiotics is essential. Current preclinical antimicrobial development yields a significant number of leads that prove unsuitable either prior to or during clinical trials. To increase the efficiency of preclinical development, relevant, standardized, accessible, and cost-effective models must be developed. Galleria mellonella (greater wax moth) larvae are widely used as an infection model to assess microbial virulence, conduct drug toxicity testing, and serve as a preliminary means of evaluating the in vivo efficacy of novel antimicrobial compounds. These infection models have greater biological relevance than many in vitro screens of comparable throughput and decrease reliance on mammalian models when used as a pre-screen for antimicrobial testing. This protocol describes a standardized methodology for the optimization of G. mellonella infection models, which can be applied to bacterial species and antimicrobial therapeutics of choice. Using the WHO priority pathogen Pseudomonas aeruginosa as an exemplar, we outline steps that can be undertaken to develop a reproducible model of infection and therapeutic testing. This includes recommendations on experimental setup, sample preparation, and infection and treatment protocols. Integration of this model within preclinical antimicrobial development pipelines would decrease reliance on mammalian models, reduce the number of ineffective compounds reaching clinical trials, and ultimately increase the efficiency of preclinical antimicrobial development.

Assessing batch variation in G. mellonella weight 
A potential source of unwanted variation in infection experiments comes from size differences between individual experimental units (i.e., larvae) and across batches. The effects of this variation can be mitigated either by adjusting treatment or infection doses based on weight, or by selecting only those larvae within a defined weight range for use in experiments. The latter adjustment is more pragmatic and is not subject to human error that might arise during dose preparation. An additional advantage of weighing the larvae is that it enables the conversion of treatment doses from those administered to larvae to their mg/kg human equivalents. To quantify variation within and across batches, three batches of 50 larvae, ordered at different times, were weighed. The mean weight in each group was 225.5 mg, 230.54 mg, and 215.86 mg, with standard deviations of 49.1 mg, 53.7 mg, and 44.3 mg, respectively (Figure 2A). Between batches, there was no significant difference in weight. Across batches, weight ranged from 107.5 mg to 341.0 mg, with a mean of 224.0 mg &#177; 49.2 mg.
To obtain reproducible results, larvae were weighed prior to experimentation and selected if their weight was 224 mg &#177; 49.2 mg, reducing the range of weight from 233.5 mg to 98.4 mg, and removing 33% of larvae. This is in line with previous work that identified significant variation in survival of larvae infected with MRSA with weight bands greater than 100 mg14,20. We also compared G. mellonella weight at the point of delivery to that at one week post-delivery, as any significant weight change could influence experimental outcomes when larvae are not used immediately upon arrival. The mean G. mellonella weight was 230.54 mg &#177; 53.7 mg. One week post-delivery, the mean weight was 221.8 mg &#177; 45.7 mg standard deviation (Figure 2B). There was no significant difference between weight on arrival and weight after one week, from which we conclude that larvae can be used for experimental purposes at any point within the first week from delivery. It is important to note that these results are representative only of G. mellonella purchased from one supplier, and weight may differ significantly between suppliers or when larvae are ordered at different times.
Optimizing inoculum density of P. aeruginosa PAO1 
The virulence of five P. aeruginosa isolates at four inoculum densities was assessed, including three commonly used laboratory strains, PAO1, PA14, and PAK, and two clinical isolates from chronic respiratory infection, LESB58, and IST27-M. These were used as part of a CF-relevant strain panel developed by Mahenthiralingam et al.21 and are representative of the global phylogeny of the species. Preliminary growth data in nutrient broth showed a lower growth rate for the isolates from chronic infection (Figure 3). Considering this, G. mellonella were infected in groups of 10 larvae with doses of 101, 102, 103, or 104 CFU/larva in 10&#956;l of PBS for PAO1, PA14, and PAK, and doses of 102, 103, 104, or 105 CFU/larva for LESB58 and IST27-M. Two groups of 10 larvae were also injected with PBS only, one group before and one group after the infections. PBS injections before infections control for contaminated PBS or contamination of needles with microbial species from the Galleria cuticle, while PBS injections after infection control for any contamination of needles with bacteria used in the infection process. Optimal doses for PAO1, PA14, and PAK were 10 CFU/larva, as greater densities resulted in &#62; 50% death by 18 h (Figure 4). 10 CFU was the lowest dose that could be reliably and reproducibly prepared for infection. Higher doses of LESB58 and IST27-M were required to achieve the desired survival kinetics, reflecting the slower growth and lower carrying capacity of these isolates under in vitro conditions&#160;(Figure 4). The optimum dose for both was 104 CFU/larvae. LESB58 and IST27-M are clinical isolates from individuals with chronic infections, and LESB58 has previously demonstrated lower virulence in rodent models than PAO122.
Toxicity testing of tobramycin and colistin in Galleria mellonella 
Before assessing the efficacy of novel antimicrobial compounds, their toxicity must be assessed by injecting a broad range of clinically relevant doses. This allows compounds with high toxicity to be removed from testing early in the preclinical pipeline. Tobramycin and colistin were assessed against uninfected G. mellonella larvae, as they are commonly administered for the treatment of P. aeruginosa infection in people with cystic fibrosis (pwCF)23. Clinical use of tobramycin ranges from 3 mg/kg daily for severely ill individuals without cystic fibrosis to 11 mg/kg every 24 h for those with cystic fibrosis24,25. These values were used as a guide for dosing in Galleria mellonella, with 1 mg/kg, 2.5 mg/kg, 5 mg/kg, 10 mg/kg, 25 mg/kg, 50 mg/kg, 100 mg/kg, 250 mg/kg tobramycin selected for toxicity testing. No death was observed at any concentration. Considering the lack of toxicity of tobramycin at high concentrations, colistin toxicity was assessed as it has previously been associated with nephro- or neuro-toxicity in 29.8% of pwCF, with a loading dose of 2.9 (&#177;1.5) mg/kg and the overall daily dose of 4.1 (&#177;1.1) mg/kg26. This made it a valuable candidate for toxicity testing, although the organ-specific effects in humans suggested the toxicity may not translate to G. mellonella. Indeed, when doses of 1 mg/kg, 2.5 mg/kg, 5 mg/kg, 10 mg/kg, 25 mg/kg, 50 mg/kg, 100 mg/kg, and 250 mg/kg of colistin were administered, no death of larvae was observed over 72 h. As such, colistin was finally administered at its highest solubility in H2O, at 2000 mg/kg. Death of all larvae was observed within 12 h, confirming that drug toxicity can be assessed in G. mellonella but that caution should be applied when trying to predict forward to human toxicity.
Optimizing treatment dosage of tobramycin against P. aeruginosa PAO1 infection 
A range of clinically relevant tobramycin doses were administered to P. aeruginosa-infected larvae to optimize treatment dosage. For novel antimicrobials, the dosage can be initially selected based on the clinical use of similar existing antibiotics or on preclinical data for the novel agent, such as broth minimum inhibitory concentrations. To assess tobramycin efficacy against P. aeruginosa PAO1, G. mellonella larvae were infected with 10 CFU of P. aeruginosa PAO1, as previously optimized, and injected with 1 mg/kg, 2.5 mg/kg, or 5 mg/kg tobramycin at 2 h post-infection. These doses were chosen based on previous G. mellonella work with tobramycin and are in line with current clinical doses of tobramycin in individuals without cystic fibrosis24,27,28.
The threshold for initial success was a 50% increase in G. mellonella survival compared to the untreated controls. PAO1 treatment with 1 mg/kg of tobramycin had little impact on G. mellonella mortality, with 90% death at 28 h post-infection (Figure 5). Treatment with 2.5 mg/kg of tobramycin delayed mortality but yielded 80% mortality overall with 5 mg/kg of tobramycin, resulting in an optimal 90% survival. The effective dose for PA14 was 5 mg/kg, but for PAK was 2.5 mg/kg. The effective dose for IST27-M was higher at 10 mg/kg, while no tested tobramycin concentration was sufficient to rescue the larvae from LESB58 infection. This trend correlated with minimum inhibitory concentration (MIC) values for tobramycin in cation-adjusted Mueller Hinton broth, in which 1 &#181;g/mL was sufficient to inhibit 90% of growth in all strains except LESB58, which had an MIC of 8 &#181;g/mL. As such, initial MIC testing can be used to indicate relative resistance between strains, though it should not be used to determine dose ranges in G. mellonella, which should be optimized separately.
Optimization of tobramycin treatment timing against P. aeruginosa PAO1 infection 
Clinical application of antibiotics does not typically occur within hours of infection but days or weeks after. Testing novel antimicrobials in this manner is unachievable in G. mellonella, as high mortality is observed within 24 h of infection with P. aeruginosa PAO1. To increase the relevance of the infection model, novel antimicrobials should be administered as late as possible during the infection. To optimize treatment timings, 5 mg/kg of tobramycin was administered to PAO1-infected G. mellonella larvae at 2 h, 4 h, 6 h, 9 h, and 12 h post-infection. Experimental success was defined as the antibiotic treatment yielding &#62;50% increase in survival compared to infection with PAO1. Treatment at 9 h and 12 h delayed mortality, though it was unable to resolve infection (Figure 6). Treatment at 2 h, 4 h and 6 h yielded survival of over 50%.
Optimisation of G. mellonella group size 
Experimental group size was calculated based on variation observed in G. mellonella survival following infection with 10 CFU / larvae of P. aeruginosa PAO1. Group size can differ based on the expected percentage change between the untreated control and treatment group in any study (Table 1). Calculations followed that which is described by Charan et al.29. The equation used is described below.
<img alt="Equation 1" src="/files/ftp_upload/67210/67210eq01.jpg" style="margin: auto;" />
Where:
&#160; &#160; &#160;<img alt="Equation 2" src="/files/ftp_upload/67210/67210eq02.jpg" style="margin: auto;" />&#160;= 1.96 at type 1 error of 5%.
&#160; &#160; &#160;Z&#946; = 0.842 is the value that provides 80% statistical power.
&#160; &#160; &#160;p1 = The proportion of events in the test group, calculated as p2 + the expected percentage change
&#160; &#160; &#160;p2 = The proportion of events in the control (untreated infection) group, calculated based on P. aeruginosa PAO1 survival variability at <img alt="Equation 3" src="/files/ftp_upload/67210/67210eq03.jpg" style="margin: auto;" />.
&#160; &#160; &#160;P = Pooled prevalence, defined as (p1 + p2)/2.
<img alt="Figure 1" class="xfigimg" src="/files/ftp_upload/67210/67210fig01.jpg" /> 
Figure 1: Schematic of a G. mellonella infection study. The general protocol involves preparation of G. mellonella larvae prior to infection, infection with 10 &#181;L inoculum, the optional treatment at a number of hours post-infection, and continuous monitoring. <a href="https://www.jove.com/files/ftp_upload/67210/67210fig01large.jpg" target="_blank">Please click here to view a larger version of this figure.</a>
<img alt="Figure 2" class="xfigimg" src="/files/ftp_upload/67210/67210fig02.jpg" /> 
Figure 2: Batch- and time-dependent variation in Galleria mellonella larvae weight.&#160;(A) Weight of three batches of 50 Galleria mellonella larvae weighed immediately upon delivery. Each batch was ordered at different times. There was no significant difference in weight across batches as calculated by a one-way ANOVA (P &#62; 0.05). (B) Weight of 50 larvae weighed upon receipt compared to the same batch weighed one week later. There was no significant difference in weight as calculated by a Student&#39;s t-test (P &#62; 0.05). ns: Not significant. <a href="https://www.jove.com/files/ftp_upload/67210/67210fig02large.jpg" target="_blank">Please click here to view a larger version of this figure.</a>
<img alt="Figure 3" class="xfigimg" src="/files/ftp_upload/67210/67210fig03.jpg" /> 
Figure 3: Growth curves of P. aeruginosa strains PAO1, PA14, PAK, LESB58, and IST27-M. Each strain was grown in LB from an initial OD600 of 0.08-0.13, and OD600 was subsequently measured every 15 min during 24 h static growth at 37&#160;&#176;C. <a href="https://www.jove.com/files/ftp_upload/67210/67210fig03large.jpg" target="_blank">Please click here to view a larger version of this figure.</a>
<img alt="Figure 4" class="xfigimg" src="/files/ftp_upload/67210/67210fig04.jpg" /> 
Figure 4: Optimization of inoculum density of Pseudomonas aeruginosa strains for infection of Galleria mellonella larvae. Survival of Galleria mellonella larvae following injection with different densities of colony-forming units (CFU) per larva. The inoculum densities tested were 10, 10&#178;, 10&#179;, or 104 CFU per larva for (A) PAO1, (B) PA14, or (C) PAK, and 10&#178;, 10&#179;, 104, or 105 CFU per larva for (D) LESB58 and (E) IST27-M. Ten larvae were used per group, each injected with 10 &#181;L of inoculum in the right rear proleg. Survival was monitored every 30 min starting 16 h post-infection, and the time of death was recorded. All strains showed dose-dependent virulence as determined by the Log-rank (Mantel-Cox) test for significance. P &#60; 0.05 for all within-strain dose comparisons except for PAK 101&#160;vs. PAK 102, PAK 103&#160;vs. PAK 104, LESB58 104&#160;vs. LESB58 105, and IST27-M 103&#160;vs. IST27-M 104, which were not significant. This figure is representative of three biological replicates. <a href="https://www.jove.com/files/ftp_upload/67210/67210fig04large.jpg" target="_blank">Please click here to view a larger version of this figure.</a>
<img alt="Figure 5" class="xfigimg" src="/files/ftp_upload/67210/67210fig05.jpg" /> 
Figure 5: Survival of Galleria mellonella larvae following injection with P. aeruginosa panel strains and treatment with tobramycin sulfate 2 h post-infection. 10 G. mellonella larvae per experimental group were infected with either 10 CFU of (A) PAO1, (B) PA14, or (C) PAK or 103 CFU of (D) LESB58 or (E) IST27-M per larvae in 10 &#181;L of PBS. Infections were administered to the rear left proleg. 2 h post-infection, PAO1, PA14, and PAK were injected with 10 &#181;L of PBS as a no-treatment control, 1 mg/kg, 2.5 mg/kg or 5 mg/kg tobramycin, with LESB58 and IST27-M treated with either 10 &#181;L PBS, 1 mg/kg, 2.5 mg/kg, 5 mg/kg, 10 mg/kg, 20 mg/kg or 40 mg/kg tobramycin, as indicated in the figure. Tobramycin was diluted in distilled water and administered in the rear right proleg. Survival was monitored continuously, and the time of death was recorded. Log-rank (Mantel-Cox) test for significance vs. the PBS control for each strain. ns: Not significant, *P &#60; 0.05, **P &#60; 0.005, ***P &#60; 0.0005 ****P &#60; 0.0001. This figure is representative of three biological replicates. <a href="https://www.jove.com/files/ftp_upload/67210/67210fig05large.jpg" target="_blank">Please click here to view a larger version of this figure.</a>
<img alt="Figure 6" class="xfigimg" src="/files/ftp_upload/67210/67210fig06.jpg" /> 
Figure 6: Survival of Galleria mellonella larvae following infection with Pseudomonas aeruginosa PAO1 and subsequent treatment with tobramycin at various time points post-infection. 10 G. mellonella larvae per experimental group were infected with 10 CFU of PAO1 in 10 &#181;L of PBS, injected into the rear right proleg. Larvae were subsequently injected at 2 h, 4 h, 6 h, 9 h, or 12 h post-infection with 5 mg/kg tobramycin sulfate in 10 &#181;L of distilled water in the rear left proleg. Survival was monitored continuously, and the time of death was recorded. Log-rank (Mantel-Cox) test for significance vs. untreated control. ***P &#60; 0.0005, ****P &#60; 0.0001. This figure is representative of three biological replicates. <a href="https://www.jove.com/files/ftp_upload/67210/67210fig06large.jpg" target="_blank">Please click here to view a larger version of this figure.</a>
<table border="1" fo:keep-together.within-page="1" fo:keep-with-next.within-page="always">
	<tbody>
		<tr>
			<td>Expected change in survival (%)</td>
			<td>Group size</td>
		</tr>
		<tr>
			<td>30</td>
			<td>26</td>
		</tr>
		<tr>
			<td>40</td>
			<td>18</td>
		</tr>
		<tr>
			<td>50</td>
			<td>13</td>
		</tr>
		<tr>
			<td>60</td>
			<td>10</td>
		</tr>
		<tr>
			<td>70</td>
			<td>8</td>
		</tr>
		<tr>
			<td>80</td>
			<td>6</td>
		</tr>
		<tr>
			<td>90</td>
			<td>5</td>
		</tr>
		<tr>
			<td>100</td>
			<td>4</td>
		</tr>
	</tbody>
</table>
Table 1: Group size for G. mellonella survival experiments in which G. mellonella larvae are infected with 10 CFU/larvae with P. aeruginosa PAO1 and subsequently administered an agent.

Author Spotlight: Characterizing Airway Environments to Advance Model Systems and Antimicrobial Discovery in Cystic Fibrosis and Chronic Respiratory Infections

This study presents a standardized framework for optimizing G. mellonella infection models for use in preclinical antimicrobial assessment. The application of a G. mellonella model as part of a preclinical antimicrobial development pipeline could decrease the number of ineffective compounds progressing to clinical trials.

Galleria mellonella as an Antimicrobial Screening Model

To combat the rising global issue of antibiotic resistance, the accelerated development of novel antibiotics is essential. Current preclinical ...

galleria-mellonella-as-an-antimicrobial-screening-model

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JoVE Journal

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1.5K Views.  University of Dundee. This study presents a standardized framework for optimizing G. mellonella infection models for use in preclinical antimicrobial assessment. The application of a G. mellonella model as part of a preclinical antimicrobial development pipeline could decrease the number of ineffective compounds progressing to clinical trials.

Video: Author Spotlight: Characterizing Airway Environments to Advance Model Systems and Antimicrobial Discovery in Cystic Fibrosis and Chronic Respiratory Infections

Microinjection of Medaka Embryos for use as a Model Genetic Organism

In this video, we demonstrate the technique of microinjection into one-cell stage medaka embryos. Medaka is a small egg-laying freshwater fish that allows both genetic and embryological analyses and is one of the vertebrate model organisms in which genome-wide phenotype-driven mutant screens were carried out 1, as in zebrafish and the mouse. Divergence of functional overlap of related genes between medaka and zebrafish allows identification of novel phenotypes that are unidentifiable in a single species 2, thus medaka and zebrafish are complementary for genetic dissection of vertebrate genome functions.
To take advantage of medaka fish whose embryos are transparent and develop externally, microinjection is an essential technique to inject cell-tracers for labeling cells, mRNAs or anti-sense oligonucleotides for over-expressing and knocking-down genes of interest, and DNAs for making transgenic lines.

Medaka and zebrafish are complementary for genetic dissection of vertebrate genome functions. This protocol highlights the key points for successful microinjection into medaka embryos, an important technique for embryological and genetic analysis using medaka and zebrafish in a laboratory.

In this video, we demonstrate the technique of microinjection into one-cell stage medaka embryos. Medaka is a small egg-laying freshwater fish that allows ...

Characterizing Herbivore Resistance Mechanisms: Spittlebugs on Brachiaria spp. as an Example

Plants can resist herbivore damage through three broad mechanisms: antixenosis, antibiosis and tolerance1. Antixenosis is the degree to which the plant is avoided when the herbivore is able to select other plants2. Antibiosis is the degree to which the plant affects the fitness of the herbivore feeding on it1.Tolerance is the degree to which the plant can withstand or repair damage caused by the herbivore, without compromising the herbivore's growth and reproduction1. The durability of herbivore resistance in an agricultural setting depends to a great extent on the resistance mechanism favored during crop breeding efforts3.
We demonstrate a no-choice experiment designed to estimate the relative contributions of antibiosis and tolerance to spittlebug resistance in Brachiaria spp. Several species of African grasses of the genus Brachiaria are valuable forage and pasture plants in the Neotropics, but they can be severely challenged by several native species of spittlebugs (Hemiptera: Cercopidae)4.To assess their resistance to spittlebugs, plants are vegetatively-propagated by stem cuttings and allowed to grow for approximately one month, allowing the growth of superficial roots on which spittlebugs can feed. At that point, each test plant is individually challenged with six spittlebug eggs near hatching. Infestations are allowed to progress for one month before evaluating plant damage and insect survival. Scoring plant damage provides an estimate of tolerance while scoring insect survival provides an estimate of antibiosis. This protocol has facilitated our plant breeding objective to enhance spittlebug resistance in commercial brachiariagrases5.

Characterizing Herbivore Resistance Mechanisms: Spittlebugs on Brachiaria spp. as an Example

This video explains mechanisms of host plant resistance to herbivory and demonstrates a no-choice test that estimates the relative contributions of antibiosis and tolerance to spittlebug resistance in Brachiaria spp.

Plants can resist herbivore damage through three broad mechanisms: antixenosis, antibiosis and tolerance1. Antixenosis is the degree to which the plant is ...

Electroantennographic Bioassay as a Screening Tool for Host Plant Volatiles

Plant volatiles play an important role in plant-insect interactions. Herbivorous insects use plant volatiles, known as kairomones, to locate their host plant.1,2 When a host plant is an important agronomic commodity feeding damage by insect pests can inflict serious economic losses to growers. Accordingly, kairomones can be used as attractants to lure or confuse these insects and, thus, offer an environmentally friendly alternative to pesticides for insect control.3 Unfortunately, plants can emit a vast number volatiles with varying compositions and ratios of emissions dependent upon the phenology of the commodity or the time of day. This makes identification of biologically active components or blends of volatile components an arduous process. To help identify the bioactive components of host plant volatile emissions we employ the laboratory-based screening bioassay electroantennography (EAG). EAG is an effective tool to evaluate and record electrophysiologically the olfactory responses of an insect via their antennal receptors. The EAG screening process can help reduce the number of volatiles tested to identify promising bioactive components. However, EAG bioassays only provide information about activation of receptors. It does not provide information about the type of insect behavior the compound elicits; which could be as an attractant, repellent or other type of behavioral response. Volatiles eliciting a significant response by EAG, relative to an appropriate positive control, are typically taken on to further testing of behavioral responses of the insect pest. The experimental design presented will detail the methodology employed to screen almond-based host plant volatiles4,5 by measurement of the electrophysiological antennal responses of an adult insect pest navel orangeworm (Amyelois transitella) to single components and simple blends of components via EAG bioassay. The method utilizes two excised antennae placed across a "fork" electrode holder. The protocol demonstrated here presents a rapid, high-throughput standardized method for screening volatiles. Each volatile is at a set, constant amount as to standardize the stimulus level and thus allow antennal responses to be indicative of the relative chemoreceptivity. The negative control helps eliminate the electrophysiological response to both residual solvent and mechanical force of the puff. The positive control (in this instance acetophenone) is a single compound that has elicited a consistent response from male and female navel orangeworm (NOW) moth. An additional semiochemical standard that provides consistent response and is used for bioassay studies with the male NOW moth is (Z,Z)-11,13-hexdecadienal, an aldehyde component from the female-produced sex pheromone.6-8

A method to rapidly screen host plant volatiles by measurement of the electrophysiological response of adult navel orangeworm (Amyelois transitella) antennae to single components and blends via electroantennographic analysis is demonstrated.

Plant volatiles play an important role in plant-insect interactions. Herbivorous insects use plant volatiles, known as kairomones, to locate their host ...

RNA Catalyst as a Reporter for Screening Drugs against RNA Editing in Trypanosomes

Substantial progress has been made in determining the mechanism of mitochondrial RNA editing in trypanosomes. Similarly, considerable progress has been made in identifying the components of the editosome complex that catalyze RNA editing. However, it is still not clear how those proteins work together. Chemical compounds obtained from a high-throughput screen against the editosome may block or affect one or more steps in the editing cycle. Therefore, the identification of new chemical compounds will generate valuable molecular probes for dissecting the editosome function and assembly. In previous studies, in vitro editing assays were carried out using radio-labeled RNA. These assays are time consuming, inefficient and unsuitable for high-throughput purposes. Here, a homogenous fluorescence-based &#8220;mix and measure&#8221; hammerhead ribozyme in vitro reporter assay to monitor RNA editing, is presented. Only as a consequence of RNA editing of the hammerhead ribozyme a fluorescence resonance energy transfer (FRET) oligoribonucleotide substrate undergoes cleavage. This in turn results in separation of the fluorophore from the quencher thereby producing a signal. In contrast, when the editosome function is inhibited, the fluorescence signal will be quenched. This is a highly sensitive and simple assay that should be generally applicable to monitor in vitro RNA editing or high throughput screening of chemicals that can inhibit the editosome function.

A highly sensitive ribozyme-based assay, applicable to high-throughput screening of chemicals targeting the unique process of RNA editing in trypanosomatid pathogens, is described in this paper. Inhibitors can be used as tools for hypothesis-driven analysis of the RNA editing process and ultimately as therapeutics.

Substantial progress has been made in determining the mechanism of mitochondrial RNA editing in trypanosomes. Similarly, considerable progress has been ...

High-throughput Screening for Chemical Modulators of Post-transcriptionally Regulated Genes

Both transcriptional and post-transcriptional regulation have a profound impact on genes expression. However, commonly adopted cell-based screening assays focus on transcriptional regulation, being essentially aimed at the identification of promoter-targeting molecules. As a result, post-transcriptional mechanisms are largely uncovered by gene expression targeted drug development. Here we describe a cell-based assay aimed at investigating the role of the 3&#39; untranslated region (3&#8217; UTR) in the modulation of the fate of its mRNA, and at identifying compounds able to modify it. The assay is based on the use of a luciferase reporter construct containing the 3&#8217; UTR of a gene of interest stably integrated into a disease-relevant cell line. The protocol is divided into two parts, with the initial focus on the primary screening aimed at the identification of molecules affecting luciferase activity after 24 hr of treatment. The second part of the protocol describes the counter-screening necessary to discriminate compounds modulating luciferase activity specifically through the 3&#8217; UTR. In addition to the detailed protocol and representative results, we provide important considerations about the assay development and the validation of the hit(s) on the endogenous target. The described cell-based reporter gene assay will allow scientists to identify molecules modulating protein levels via post-transcriptional mechanisms dependent on a 3&#8217; UTR.

Here we describe a cell-based reporter gene assay as a valuable tool to screen chemical libraries for compounds modulating post-transcriptional control mechanisms exerted through 3&#8217; UTR.

Both transcriptional and post-transcriptional regulation have a profound impact on genes expression. However, commonly adopted cell-based screening assays ...

Xenopus laevis as a Model to Identify Translation Impairment

Protein synthesis is a fundamental process to gene expression impacting diverse biological processes notably adaptation to environmental conditions. The initiation step, which involves the assembly of the ribosomal subunits at the mRNA initiation codon, involved initiation factor including eIF4G1. Defects in this rate limiting step of translation are linked to diverse disorders. To study the potential consequences of such deregulations, Xenopus laevis oocytes constitute an attractive model with high degrees of conservation of essential cellular and molecular mechanisms with human. In addition, during meiotic maturation, oocytes are transcriptionally repressed and all necessary proteins are translated from preexisting, maternally derived mRNAs. This inexpensive model enables exogenous mRNA to become perfectly integrated with an effective translation. Here is described a protocol for assessing translation with a factor of interest (here eIF4G1) using stored maternal mRNA that are the first to be polyadenylated and translated during oocyte maturation as a physiological readout. At first, mRNA synthetized by in vitro transcription of plasmids of interest (here eIF4G1) are injected in oocytes and kinetics of oocyte maturation by Germinal Vesicle Breakdown detection is determined. The studied maternal mRNA target is the serine/threonine-protein-kinase mos. Its polyadenylation and its subsequent translation are investigated together with the expression and phosphorylation of proteins of the mos signaling cascade involved in oocyte maturation. Variations of the current protocol to put forward translational defects are also proposed to emphasize its general applicability. In light of emerging evidence that aberrant protein synthesis may be involved in the pathogenesis of neurological disorders, such a model provides the opportunity to easily assess this impairment and identify new targets.

Xenopus laevis as a Model to Identify Translation Impairment

Protein synthesis control occurs mainly at the translation initiation step, deficiencies in which are linked to diverse disorders. To better understand their etiology, we described here a protocol using Xenopus laevis oocytes assessing the translation of mos transcript in the presence of a mutant of translation initiation factor eIF4G1.

Protein synthesis is a fundamental process to gene expression impacting diverse biological processes notably adaptation to environmental conditions. The ...

Comet Assay as an Indirect Measure of Systemic Oxidative Stress

Higher eukaryotic organisms cannot live without oxygen; yet, paradoxically, oxygen can be harmful to them. The oxygen molecule is chemically relatively inert because it has two unpaired electrons located in different pi * anti-bonding orbitals. These two electrons have parallel spins, meaning they rotate in the same direction about their own axes. This is why the oxygen molecule is not very reactive. Activation of oxygen may occur by two different mechanisms; either through reduction via one electron at a time (monovalent reduction), or through the absorption of sufficient energy to reverse the spin of one of the unpaired electrons. This results in the production of reactive oxidative species (ROS). There are a number of ways in which the human body eliminates ROS in its physiological state. If ROS production exceeds the repair capacity, oxidative stress results and damages different molecules. There are many different methods by which oxidative stress can be measured. This manuscript focuses on one of the methods named cell gel electrophoresis, also known as &#8220;comet assay&#8221; which allows measurement of DNA breaks. If all factors known to cause DNA damage, other than oxidative stress are kept constant, the amount of DNA damage measured by comet assay is a good parameter of oxidative stress. The principle is simple and relies upon the fact that DNA molecules are negatively charged. An intact DNA molecule has such a large size that it does not migrate during electrophoresis. DNA breaks, however, if present result in smaller fragments which move in the electrical field towards the anode. Smaller fragments migrate faster. As the fragments have different sizes the final result of the electrophoresis is not a distinct line but rather a continuum with the shape of a comet. The system allows a quantification of the resulting &#8220;comet&#8221; and thus of the DNA breaks in the cell.

Comet assay measures DNA breaks, induced by different factors. If all factors (except oxidative stress) causing DNA damage are kept constant, the amount of DNA damage is a good indirect parameter of oxidative stress. The goal of this protocol is to use comet assay for indirect measurement of oxidative stress.

Higher eukaryotic organisms cannot live without oxygen; yet, paradoxically, oxygen can be harmful to them. The oxygen molecule is chemically relatively ...

Experimental Protocol for Using Drosophila As an Invertebrate Model System for Toxicity Testing in the Laboratory

Emergent properties and external factors (population-level and ecosystem-level interactions, in particular) play important roles in mediating ecologically-important endpoints, though they are rarely considered in toxicological studies. D. melanogaster is emerging as a toxicology model for the behavioral, neurological, and genetic impacts of toxicants, to name a few. More importantly, species in the genus Drosophila can be utilized as a model system for an integrative framework approach to incorporate emergent properties and answer ecologically-relevant questions in&#160;toxicology research. The aim of this paper is to provide a protocol for exposing species in the genus Drosophila to pollutants to be used as a model system for a range of phenotypic outputs and ecologically-relevant questions. More specifically, this protocol can be used to 1) link multiple biological levels of organization and understand the impact of toxicants on both individual- and population-level fitness; 2) test the impact of toxicants at different stages of developmental exposure; 3) test multigenerational and evolutionary implications of pollutants; and 4) test multiple contaminants and stressors simultaneously.

Experimental Protocol for Using Drosophila As an Invertebrate Model System for Toxicity Testing in the Laboratory

In this paper, we provide a detailed protocol for exposing species in the genus Drosophila to pollutants with the goal of studying the impact of exposure on a range of phenotypic outputs at different developmental stages and for more than one generation.

Emergent properties and external factors (population-level and ecosystem-level interactions, in particular) play important roles in mediating ...

Mass Spectrometry Analysis to Identify Ubiquitylation of EYFP-tagged CENP-A (EYFP-CENP-A)

Studying the structure and the dynamics of kinetochores and centromeres is important in understanding chromosomal instability (CIN) and cancer progression. How the chromosomal location and function of a centromere (i.e., centromere identity) are determined and participate in accurate chromosome segregation is a fundamental question. CENP-A is proposed to be the non-DNA indicator (epigenetic mark) of centromere identity, and CENP-A ubiquitylation is required for CENP-A deposition at the centromere, inherited through dimerization between cell division, and indispensable to cell viability.
Here we describe mass spectrometry analysis to identify ubiquitylation of EYFP-CENP-A K124R mutant suggesting that ubiquitylation at a different lysine is induced because of the EYFP tagging in the CENP-A K124R mutant protein. Lysine 306 (K306) ubiquitylation in EYFP-CENP-A K124R was successfully identified, which corresponds to lysine 56 (K56) in CENP-A through mass spectrometry analysis. A caveat is discussed in the use of GFP/EYFP or the tagging of high molecular weight protein as a tool to analyze the function of a protein. Current technical limit is also discussed for the detection of ubiquitylated bands, identification of site-specific ubiquitylation(s), and visualization of ubiquitylation in living cells or a specific single cell during the whole cell cycle.
The method of mass spectrometry analysis presented here can be applied to human CENP-A protein with different tags and other centromere-kinetochore proteins. These combinatory methods consisting of several assays/analyses could be recommended for researchers who are interested in identifying functional roles of ubiquitylation.

Mass Spectrometry Analysis to Identify Ubiquitylation of EYFP-tagged CENP-A EYFP-CENP-A

CENP-A ubiquitylation is an important requirement for CENP-A deposition at the centromere, inherited through dimerization between cell division, and indispensable to cell viability. Here we describe mass spectrometry analysis to identify ubiquitylation of EYFP-tagged CENP-A (EYFP-CENP-A) protein.

Studying the structure and the dynamics of kinetochores and centromeres is important in understanding chromosomal instability (CIN) and cancer ...

Tobacco Hornworm as an Insect Model System for Cannabinoid Pre-clinical Studies

With increased attention on cannabinoids in medicine, several mammalian model organisms have been used to elucidate their unknown pharmaceutical functions. However, many difficulties remain in mammalian research, which necessitates the development of non-mammalian model organisms for cannabinoid research. The authors suggest the tobacco hornworm Manduca sexta as a novel insect model system. This protocol provides information on preparing the artificial diet with varying amounts of cannabidiol (CBD), setting up a cultivation environment, and monitoring their physiological and behavioral changes in response to CBD treatment. Briefly, upon receiving hornworm eggs, the eggs were allowed 1-3 days at 25 &#176;C on a 12:12 light-dark cycle to hatch before being randomly distributed into control (wheat germ-based artificial diet; AD), vehicle (AD + 0.1% medium-chain triglyceride oil; MCT oil) and treatment groups (AD + 0.1% MCT + 1 mM or 2 mM of CBD). Once the media was prepared, 1st instar larvae were individually placed in a 50 mL test tube with a wooden skewer stick, and then the test tube was covered with a cheesecloth. Measurements were taken in 2-day intervals for physiological and behavioral responses to the CBD administration. This simple cultivation procedure allows researchers to test large specimens in a given experiment. Additionally, the relatively short life cycles enable researchers to study the impact of cannabinoid treatments over multiple generations of a homogenous population, allowing for data to support an experimental design in higher mammalian model organisms.

The present protocol provides instructional information for using tobacco hornworm Manduca sexta in cannabinoid research. The method described here includes all necessary supplies and protocols to monitor physiological and behavioral changes of the insect model in response to cannabidiol (CBD) treatment.