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PLoS One. 2017; 12(3): e0173362.
Published online 2017 March 9. doi:  10.1371/journal.pone.0173362
PMCID: PMC5344393

Systemic thioridazine in combination with dicloxacillin against early aortic graft infections caused by Staphylococcus aureus in a porcine model: In vivo results do not reproduce the in vitro synergistic activity

Tom Coenye, Editor



Conservative treatment solutions against aortic prosthetic vascular graft infection (APVGI) for inoperable patients are limited. The combination of antibiotics with antibacterial helper compounds, such as the neuroleptic drug thioridazine (TDZ), should be explored.


To investigate the efficacy of conservative systemic treatment with dicloxacillin (DCX) in combination with TDZ (DCX+TDZ), compared to DCX alone, against early APVGI caused by methicillin-sensitive Staphylococcus aureus (MSSA) in a porcine model.


The synergism of DCX+TDZ against MSSA was initially assessed in vitro by viability assay. Thereafter, thirty-two pigs had polyester grafts implanted in the infrarenal aorta, followed by inoculation with 106 CFU of MSSA, and were randomly administered oral systemic treatment with either 1) DCX or 2) DCX+TDZ. Treatment was initiated one week postoperatively and continued for a further 21 days. Weight, temperature, and blood samples were collected at predefined intervals. By termination, bacterial quantities from the graft surface, graft material, and perigraft tissue were obtained.


Despite in vitro synergism, the porcine experiment revealed no statistical differences for bacteriological endpoints between the two treatment groups, and none of the treatments eradicated the APVGI. Accordingly, the mixed model analyses of weight, temperature, and blood samples revealed no statistical differences.


Conservative systemic treatment with DCX+TDZ did not reproduce in vitro results against APVGI caused by MSSA in this porcine model. However, unexpected severe adverse effects related to the planned dose of TDZ required a considerable reduction to the administered dose of TDZ, which may have compromised the results.


Aortic prosthetic vascular graft infection (APVGI) is a serious and therapeutically challenging complication. In earlier series, mortality and lower-limb amputation rates are reportedly up to 88% and 25%, respectively [13]. Methicillin-sensitive Staphylococcus aureus (MSSA) is the most frequently isolated bacteria in the early phase (≤4 months) of APVGIs, accounting for 43–64% of the isolates [4, 5]. New treatment regimens involving complete in situ graft replacement with an autogenous conduit or allograft have lowered mortality and reinfection rates considerably [1, 6]. Nonetheless, patients with APVGIs are often elderly with comorbidities, who may not be eligible for open surgery. Furthermore, an increasing number of inoperable patients are treated with endovascular aortic repair (EVAR), and infections related to endoprosthetic grafts in this category of patients render them less favourable for open surgery. Consequently, conservative treatment with antibiotic only and complete graft preservation in high risk patients has been evaluated with limited rates of success [710]. The insufficient effect of conservative APVGI treatment is probably a combination of low antibiotic bioavailability at the infection site and the formation of a protective biofilm layer, which significantly reduces the susceptibility of the microorganism [11, 12]. The use of a helper compound, such as the antipsychotic drug thioridazine (TDZ), can significantly potentiate the antibacterial efficacy of β-lactam antibiotics against both methicillin-resistant and susceptible S. aureus strains and induces a synergetic effect in vitro [1316]. On the other hand, conflicting results have been obtained in animal studies comprising C. elegans and mice [1719]. The antibacterial mechanisms of TDZ are not completely understood, but it is known to induce major changes in transcription of genes related to pathways in cell wall biosynthesis [20, 21]. Furthermore, static in vitro experiments indicate that TDZ reduces staphylococcal biofilm formation by inactivation of efflux pumps [22] and enhanced loading capacity of DCX when co-loaded with TDZ into a polymer hybrid silicone material [23], making the combination of TDZ and a β-lactam antibiotic a particularly interesting option for the management of APVGIs caused by S. aureus.

The aim of this study was to investigate the efficacy of conservative systemic treatment of TDZ in combination with dicloxacillin (DCX), compared to DCX alone, against early APVGI caused by MSSA in a porcine model. Initially, we determined the in vitro efficacy of combining DCX and TDZ against the MSSA test strain. The in vivo efficacy was evaluated primarily in terms of bacteriological endpoints and secondarily by changes in weight, temperature, white blood cell count (WBC), haemoglobin, and haptoglobin. Finally, we report on observations concerning animal welfare, treatment compliance, and adverse drug effects.

Materials and methods

Antimicrobial agents

For the in vitro experiments we used DCX (Sigma-Aldrich Corporation, Denmark) and TDZ (thioridazine hydrochloride, Sigma-Aldrich Corporation, Denmark) in its racemic form. For the in vivo experiments DCX capsules (Dicillin® 250 mg; Sandoz, Denmark) were purchased and used as commercially registered in Denmark for clinical use [24]. The purchase of TDZ tablets (Thioridazin-neuraxpharm® 25 mg; thioridazine hydrochloride, Neuraxpharm, Germany) was licenced by the Danish Health and Medicines Authority (reference no.: 2013041542).

Bacterial test strain

Throughout this study, MSSA (ATCC 29213) was utilized. This strain had previously been used and validated by Gao et al. in a similar porcine model [2527]. The strain was susceptible to oxacillin, gentamicin, ciprofloxacin, rifampicin, vancomycin and cefoxitin, but resistant to penicillin.

MIC, MBC and viability assay

Minimal inhibitory concentration (MIC) and minimum bactericidal concentration (MBC) tests were respectively performed for DCX and TDZ according to Clinical Laboratory Standards Institute guidelines, and effects on bacterial growth of DCX and TDZ alone and in combination were tested by a viability assay as previously reported by Klitgaard and colleagues [13].


We used domestic female pigs from a specific-pathogen-free herd at the Department of Animal Science, Aarhus University. All pigs were approximately three and half months old at the beginning of the experiment. During the entire study period the pigs were housed individually in pens with saw-dusted solid floors and drinking nipples. They were fed three times daily. All pigs were acclimatized under these conditions for at least one week before initiation of the experiment. The animal study protocol was approved by the Danish Animal Experimentation Inspectorate (license no. 2012-15-2934-00290).

The APVGI porcine model

The APVGI porcine model was carried out as a part of a tandem project performed in the same series of pigs involving a central venous catheter infection model [23]. Inoculation and implantation of the aortic grafts and central venous catheters were performed during the same operation using the same MSSA strain (ATCC 29213).

The anaesthetic and surgical procedure has previously been described [2527]. In brief, pigs were placed in a supine position and the surgical area was prepared with alcohol-based chlorhexidine and sterile dressings. All pigs were given a single dose of cefuroxime 1500 mg intravenously immediately before skin incision. The abdominal aorta was exposed through a 25–30 cm long midline laparotomy and the lumbar and inferior mesenteric arteries were clipped and cut. After an intravenous administration of 5000 IU of heparin, the aorta was clamped and the infrarenal aorta was replaced by an approximately 5 cm long collagen coated knitted polyester graft (Gelsoft 8 mm; Vascutek) by end-to-end anastomoses using 4–0 polypropylene sutures. Haemostasis was secured and the surface of the graft was directly inoculated with 106 CFUs of MSSA (ATTC 29219) in 0.3 mL saline solution using a 1-mL syringe. Hereafter, the retroperitoneum and abdominal wall were closed in layers with standard surgical techniques. All pigs received analgesic treatment with intramuscular injections of flunixin 150 mg with 24-hour intervals and buprenorphine 0.6 mg with 8-hour intervals for the first three days after surgery. The day of treatment initiation was defined as baseline (day 0) and therefore the day of the operation was defined as day -7. Weight and rectal temperature were measured and blood samples were collected before the operation (day -7) and at day -6 (only temperature), -5 (not weight), 0, 7, 14, and 21. These parameters were always obtained in the morning prior to treatment administration. Healthy pigs gain approximately 0.5–1.0 kilogram per day and have a normal rectal temperature range of 38.7–39.8 Celsius [28]. The blood samples were used for analysis of white blood cell count (WBC), haemoglobin (HGB) and haptoglobin—the latter being an infection marker in pigs and equivalent to C-reactive protein (CRP) in humans. A decrease in HGB and an increase in WBC and haptoglobin were interpreted as signs of an ongoing infection. Moreover, the animal keepers recorded several other parameters on an ordinal scale, such as stool (yes/no), movement (normal/impaired/abnormal), wound appearance (no infection/superficial infection/severe infection), and treatment compliance (eaten/partially eaten/not eaten/no treatment given) on a daily basis.

Treatment groups, dosages, and administration

Based on human equivalent dosages we initially planned to use a TDZ dosage of 300 mg x 2 daily, which was equivalent to 10 mg/kg/day in a 60 kg pig [29]. However, this had to be considerably reduced due to adverse drug effects. The final treatment regimens used are described below. The drugs were administered orally in two different treatment groups: 1) DCX (Dicillin 750 mg twice daily) and 2) DCX+TDZ (Dicillin 750 mg twice daily + Thioridazin-neuraxpharm 50 mg twice daily the first four days (day 0–4) and 100 mg twice daily for the rest of the treatment period (day 5–21). To enhance compliance the capsules/tablets were broken/crushed and mixed with dog food and regular pig food. Treatment was initiated 7 days after the implantation and inoculation of the aortic graft (day 0) and continued for a further 21 days. The pigs were consecutively allocated to the treatment groups by a fixed randomisation key (1, 2, 2, 1, 1, 2,…) and the animal keepers selected the pigs for surgery blinded from this random allocation.

Sampling and microbiological analyses

After 21 days of treatment, the pigs were anesthetized and the aortic graft was exposed through the previous incision under aseptic conditions. A swab with a cotton stick was done from the surface of the graft and placed in a tube with 1 mL PBS + 0,1% Triton X-100 (Sigma-Aldrich Corporation, Denmark). Tissue from the perigraft area was randomly sampled and transferred to a plastic tube with 10 ml isotonic saline (Amgros, Denmark). The aorta was ligated above and beneath the aortic graft and a minimum of 3 cm of the graft was cut out and transferred to a plastic tube with 40 ml of isotonic saline. Finally, the pigs were euthanized with an intravenous injection of phenobarbital.

Immediately, the samples were transferred to the laboratory for microbiological analysis. The swab was vortexed for one minute, and the cotton stick was wiped off on the inside of the tube before removal. Under aseptic conditions, 1 cm of the graft was cut off and placed in a tube with 5 ml PBS + 0.1% Triton X-100 and vortexed for 1 min. The tissue was weighed and homogenized in 10 ml of isotonic saline. All three solutions from the swab, tissue and graft were individually plated on Mueller-Hinton agar plates in ten-fold serial dilutions for CFU determination with 0.1 ml on each plate.

Statistical analyses

Bacterial count data from all three primary bacteriological endpoints (graft, swab, and tissue) were converted into CFU/mL and added by one (+1) to avoid zeros and allow transformation by natural logarithm (ln). Despite different transformation attempts of the data a normal distribution could not be achieved and thus, a two-sample Wilcoxon rank-sum (Mann-Whitney) test was used for comparison. Furthermore, bacterial quantity data from each bacteriological endpoint were converted into binary categorical variable and labelled: “No growth” or “Growth” referring to CFU/mL = 0 or CFU/mL>0, respectively and compared by two-sided Fisher’s exact test. Mixed models were used in the analysis of longitudinal continuous variables (weight, temperature, WBC, HGB, and haptoglobin) to pursue individual changes within treatment groups over time. Determination of the mixed model was based on the research question alone. Treatment group and time (including interaction) were set as fixed values, and baseline values (day 0) as covariates. Pig number (ID) was set as the random intercept. Ordinal outcomes of the variables: defecation, movement, wound healing, and treatment compliance were compared between treatment groups by a Chi-squared test. A p-value of <0.05 was considered significant. Stata/IC version 13.1 (Statacorp) was used for illustrations and analyses.

Sample size calculation

Sample size of the study was set upon a power calculation to detect a 50% difference in the frequency of graft infections or a 15% difference in bacterial quantities with an 80% power and a 5% significance level, assuming that 100% of the grafts will be infected by the end of the study in pigs from the control group (DCX treatment only).


MIC, MBC and viability assay

DCX and TDZ had MIC/MBC-values of 0.5/2 mg/L and 32/64 mg/L, respectively. Results of the in vitro viability assays are presented in Fig 1. In accordance with the MIC/MBC value the growth of our MSSA test strain was not inhibited by TDZ (16 mg/L) and revealed the same growth pattern as for the control (no drug). DCX (0.25 mg/L) slightly affected growth and may therefore be characterised as a sub-inhibitory concentration. However, the combination of DCX (0.25 mg/L) and TDZ (16 mg/L) showed a significant and synergetic inhibition of growth with a reduction of bacterial load of approximately 3 and 4.5 log10 CFU compared to DCX (0.25 mg/L) or TDZ (16 mg/L) alone, respectively, after 10 hours.

Fig 1
In vitro viability assay: The effect of thioridazine (TDZ) and dicloxacillin (DCX), alone and in combination, on survival of MSSA (ATCC 29213) over time.

The APVGI porcine model

According to the sample size calculation, 32 pigs were included. Seventeen pigs were allocated to the combination treatment (DCX+TDX) and 15 pigs to monotherapy (DCX). Three pigs had to be euthanized before the end of the experiment: two pigs on day 2 due to spinal cord ischemia (both allocated to the combination treatment), and one pig on day 21 due to persistent high fever (allocated to the DCX-group). In total, 29 pigs (91%) survived until the end of the experiment with a treatment group distribution of 14 pigs in the DCX-group and 15 pigs in DCX+TDZ-group. Baseline characteristics before treatment initiation (day 0) of all pigs were recorded and sorted by treatment group as presented in Table 1. Comparisons of the treatment groups revealed non-significant p-values for all parameters.

Table 1
Baseline characteristics, listed for all pigs and by treatment group.

Primary bacteriological endpoints

Following three weeks of conservative treatment with either DCX alone or DCX+TDZ in combination we determined the bacterial quantities from graft surface swabs, graft materials and perigraft tissue. As shown in Table 2, we found no statistically significant differences in bacterial quantities between the two treatment groups with respect to graft (p = 0.209), swab (p = 0.864), and tissue (p = 0.728). Some bacterial endpoints actually revealed zero bacterial counts, and therefore we decided to transform the continuous count data into binary outcomes of growth vs. no growth for a post hoc analysis. However, we still observed no significant difference between the treatment groups. Some of the microbiological analyses were inconclusive due to contamination of the agar plates and were excluded from the analysis. The number of included observations (N) from each treatment group is displayed in Table 2.

Table 2
Primary bacteriological endpoints.

Secondary longitudinal continuous outcomes

Changes in mean weight, temperature, WBC, HGB, and haptoglobin during the experimental period for both treatment groups are illustrated in Fig 2A–2E.

Fig 2
Changes in weight (A), temperature (B), white blood cell count (WBC) (C), haemoglobin (HGB) (D), and haptoglobin (E) of each treatment group during the experimental period are displayed as mean values with standard deviation bars at predefined time points. ...

Overall, the curves of the two treatment groups had similar shapes and slopes with overlapping standard deviations on all variables. However, the curves of weight, temperature, and haptoglobin slightly diverged from day 0 to day 21, meaning that the DCX-group tended to have a higher weight and temperature, but a lower level of haptoglobin than the DCX+TDZ-group toward the end of the treatment period. Furthermore, it is noteworthy that most variables improved from treatment initiation on day 0 (marked by the grey dotted line) and onwards, even though WBC increased in both treatment groups from day 0 to 7 and then decreased from day 7 to 21, and similar HGB initially improved from day 0 to 7 and then declined from day 7 to 21 (Fig 2C and Fig 2D).

Individual changes of each response variable within treatment groups over time were pursued by mixed model analysis and the coefficients are listed in Table 3.

Table 3
Mixed model analysis of longitudinal continuous outcomes.

All mixed model analyses in Table 3 are based on the DCX-group as the reference treatment group, and because no numeric conversions were made the coefficients are equivalent to the entities of each variable. The coefficients are best explained by using the response variable weight as an example. The first coefficient in the weight column explains the difference between the DCX+TDZ-group and DCX-group at the first time point after baseline, in this case day 7 (DCX+TDZ–DCX | day 7 = -1.59 kg). The next two coefficients explain the weight changes over time of the reference treatment group (DCX) compared to the measurement at day 7 and day 14, respectively (Day 14 –Day 7 | DCX = 7.32 kg; Day 21 –Day 7 | DCX = 11.34 kg. Both time points showed a highly significant increase in weight compared to day 7 (p≤0.001). The following two coefficients explain the difference between the two treatment groups at day 14 and 21 compared to the difference at day 7. Therefore, to calculate the absolute difference at day 14 and 21, the first coefficient at day 7 must be added (DCX+TDZ–DCX |day 14 = -0.99 + (-1.59) = -2.58 kg; DCX+TDZ–DCX |day 21 = -0.77 + (-1.59) = -2.36 kg.

In general, the response variables changed during the treatment period, and the last measurements on day 21 were significantly different from the first measurements after baseline (day 7) in all response variables. However, the analyses for all response variables presented no statistical significant differences between the treatment groups. The coefficients in Table 3 roughly correspond to the graphed changes in weight, temperature, WBC, HGB, and haptoglobin in Fig 2A–2E. However, they are not directly comparable since they are based on two different statistical analyses and calculations.

Animal welfare and treatment compliance

Over the complete experimental period, the daily registrations of parameters concerning animal welfare—that is, stool (yes/no), movement (normal/impaired/abnormal), and wound appearance (no infection/superficial infection/severe infection)—included 413 observations in the DCX-group and 420 observations in the DCX-TDZ-group. The DCX+TDZ group had two observations of “no stool”, but all other observations showed daily stools with no significant difference between the treatment groups (p = 0.161). We registered 14 and 21 observations of impaired movement in the DCX- and DCX+TDZ-groups, respectively. No observations were categorized as abnormal movement in the DCX-group and only 1 in the DCX+TDZ-group. Overall, we found no significant difference in the movement parameter between the treatment groups (p = 0.310). Regarding wound appearance, signs of a superficial infection were evident in 15 and 21 observations in the DCX- and DCX+TDZ-groups, respectively. Signs of severe infection were not observed in the DCX-group and only once in the DCX+TDZ-group. Overall, the chi-squared test showed no significant difference in wound appearance between the treatment groups (p = 0.379).

Registration of treatment compliance (eaten/partially eaten/not eaten/no treatment given) during the three-week treatment period included 309 observations in the DCX-group and 315 observations in the DCX-TDZ-group. In the DCX-group, the treatment was eaten in 298/309 (96%) observations and only partially or not eaten in 8 and 3 observations, respectively. In the DCX+TDZ-group, the treatment was eaten in 296/315 (94%) observations and only partially or not eaten in 11 and 8 observations, respectively. There were no observations of “no treatment given” in any of the treatment groups. Overall, we found high treatment compliance in both groups with no statistical difference (p = 0.263).

Adverse drug effects

Shortly after treatment initiation in the pilot study, we observed unexpected severe extrapyramidal adverse effects and behavioural changes in the pigs treated with a TDZ dose of 300 mg x 2 daily in combination with DCX. The pigs showed signs varying from dizziness and drowsiness to severe agitation with repetitive compulsive self-destructive behaviour (e.g. licking or scratching the same spot of the pen walls for several hours resulting in abrasions to the head or snout). Pigs treated with DCX alone showed no signs of these behavioural changes. In consultation with the supervisory veterinarian, we gradually reduced the dosage of TDZ until these adverse effects were acceptable in relation to animal welfare and ethical regulations. A TDZ dose reduction to less than a third of the initial dose was required to reach acceptably low levels of side effects.


This study is the first large-animal model investigation of TDZ used in combination with a β-lactam antibiotic as conservative systemic treatment against a vascular graft infection caused by S. aureus. Our in vitro experiments were able to reproduce the previously demonstrated in vitro synergy of DCX and TDZ against the chosen MSSA test strain, but in our porcine model the combination treatment failed to eradicate early APVGI caused by 106 CFU of MSSA after three weeks of conservative systemic treatment. Based on the bacterial quantities of the three primary bacteriological endpoints, no statistical potentiated or synergetic effect of the combination treatment was found compared to treatment with DCX alone. We emphasize that both treatment groups had high treatment compliance with no statistical difference and therefore, this factor can be ruled out as a potential bias.

Before treatment initiation all pigs showed increasing temperature and haptoglobin and decreasing HBG within the first week after graft implantation and inoculation (Fig 2B, Fig 2D, and Fig 2E), indicating that APVGI was successfully and consistently established.

The bacteriological results had quite wide ranges, and a few samples within each bacteriological endpoint even showed no bacterial growth, but these findings were present in both treatment groups with no statistical difference (Table 2). Gao et al. [27], who used the same APVGI porcine model, bacterial strain and inoculum concentration, also reported large SDs in bacterial load on graft material of 2.93 (SD: 1.45) log10 CFU equivalent to 6.75 (SD: 3.34) ln CFU following a treatment regimen, which also failed to eradicate the graft infection. This indicates that insufficient antimicrobial treatment enhances the influence of intrinsic biological variations, which can be expressed as large SDs of quantitative bacteriological endpoints, as seen in our study.

Most secondary outcomes improved after treatment initiation, indicating some effect of both treatments, including small differences (especially for weight, temperature, and haptoglobin) between the treatment groups (Fig 2A–2E). However, the mixed model analyses of all secondary outcomes revealed no significant individual differences between treatment groups during the treatment period.

Our results are in accordance with the findings of two recent animal studies addressing the potential of systemic treatment with TDZ in combination with a β-lactam antibiotic against S. aureus [18, 19]. We have recently published assessments of TDZ as a helper compound to DCX against methicillin-resistant S. aureus (MRSA) in a modified mouse peritonitis model [18]. No synergetic effect was found using subcutaneous systemic treatment; however, increased systemic dosages of DCX+TDZ revealed an underpowered tendency towards better antimicrobial efficacy but also indications of increasing adverse effects [18]. Hahn and colleagues [19] also failed to show any synergetic effect with systemic treatment (intraperitoneal and subcutaneous administration) of TDZ in combination with cefazolin against MRSA and MSSA in a mouse skin infection model. No adverse effects were reported.

In contrast, in vivo synergy of TDZ+DCX against MRSA was confirmed in a C. elegans model [17] and by local intraperitoneal administration in our modified mouse peritonitis model [18]. It is noteworthy that the presence of high drug concentrations directly at the infection site is a recurrent characteristic of these two model designs, and all other animal studies reporting positive outcomes of the treatment with TDZ alone or in combination with an antibiotic [17, 18, 23, 3033].

The promising in vitro results presented here and in a recently published paper [23], along with the previous report of TDZ’s anti-biofilm capacity [22], led us to this intriguing idea of TDZ in combination with a β-lactam antibiotic as a possible new conservative treatment solution against APVGI caused by MSSA. However, the in vitro activities did not manifest in this in vivo model using systemic treatment in non-toxic dosages. The reason for this discrepancy is unknown, but the following speculations could guide the design of further investigations to clarify the issue. First, we recognize that APVGI is arguably one of the most difficult infections to eradicate without supplemental surgical intervention, and so far, no valid alternative is available. Furthermore, we may have used inadequate dosages of DCX. More frequent daily dosages and intravenous administration were also initially considered, but this was not feasible under the given experimental conditions. Unexpected severe adverse effects related to the planned TDZ dose forced us to use a substantially lower dose of TDZ. This may have compromised the results when compared to the in vitro analyses, but these pre-clinical observations are also vital to protect human patients. Thus, these unexpected findings highlight the importance of performing pre-clinical investigations in higher ranked animals such as pigs, which are physiologically and genetically more similar to humans than rodents [34].

Some reports have demonstrated the ability of TDZ to concentrate in macrophages, which is mediated by lysosomal trapping [3537], and we speculate that infections occurring in macrophage-rich tissue, such as lung, kidney, and liver, may be better suited for systemic treatment with this drug combination. In support of this possibility, Hahn et al. demonstrated reduced bacterial dissemination to the spleen and kidneys [19]. However, further animal pharmacodynamic studies are needed to clarify TDZ’s penetration, uptake, and distribution in various tissues and the impact of infection and inflammation on these parameters.

Another explanation of the in vitro/in vivo discrepancy is the possibility of a drug-drug interaction between TDZ and DCX. A pharmaco-epidemiologic study has recently confirmed previous reports on DCX’s ability to decrease the effect of liver metabolised drugs such as warfarin [38]. This interaction is most likely mediated through DCX’s activation of the pregnane X receptor, resulting in induction of CYP3A4 [39], which in combination with CYP2D6, significantly contributes to the metabolism of TDZ [40]. Furthermore, a recent report indicates that pigs are fast metabolisers of CYP2D6 substrates [41]. Hence, co-administration of DCX and TDZ in pigs may result in an increased conversion of TDZ into metabolites with potentially lower or no antibacterial activity, but which retain potent neuroleptic effects [42]. This could also explain the observed lack of antimicrobial synergy and the unexpected severe neurologic side effects at dosages which, from human clinical experience, ought to be well-tolerated.

Evidently, this limits the potential of TDZ as an antimicrobial helper compound for systemic treatment. However, TDZ as a helper compound to an antibiotic drug could still be useful for local or topical treatment, for example as part of antimicrobial impregnations of indwelling medical devices or antibacterial ointments against staphylococcal skin infections. We have just recently published a study showing that the combined loading of DCX + TDZ into a polymer hybrid silicone catheter material increased the antibacterial efficiency, although release analyses revealed that this effect was caused by a change in loading kinetics and an enhanced loading capacity of DCX facilitated by the presence of TDZ [23]. Moreover, the purified (-) enantiomer of TDZ, also patented under the name JEK47, apparently exhibits a more favourable toxic profile than its racemate, while maintaining the same antibacterial activity [43]. JEK47 is a promising agent, although in vivo evidence of its combined activity with DCX is still lacking.

The idea of enhancing the antimicrobial activity of antibiotics with helper compounds is far from exhausted. Several other prospects of antimicrobial helper compounds, which share chemical structural resemblance with phenothiazines, have been identified and investigated as adjuncts to different antibiotics against S. aureus. A screening for antimicrobial activity of 1,057 previously approved drugs derived from the WHO and US Food and Drug Administration drug lists, revealed a total of 69 potential non-antibiotic helper compounds that potentiate the antimicrobial activity of a semi-synthetic tetracycline (minocycline) in vitro [44]. Thirty-five out of the 69 identified helper compounds demonstrated synergism in combination with minocycline against S. aureus. Especially, disulfiram (also known as: Antabus) showed a strong synergetic effect on growth inhibition of both MSSA and MRSA strains, including USA300 [44]. Furthermore, chemically designed 2-Phenylquinolines derivatives have proven to be a potent new class of S. aureus NorA efflux pump inhibitors [45], and studies on β-lactams in combination with cyslabdan, produced by Streptomyces sp. K04-0144, have also revealed a considerable reduction in MICs against MRSA [46, 47].

In summary, combining drugs to combat antimicrobial resistance is an intriguing field with a great clinical potential. However, at the same time it adds to biological complexity, both in regard to clinical efficacy and host toxicity, thus in vivo studies are demanded. The findings from this study underline the importance of performing in vivo studies in large animal models, which to the highest possible degree mimic conditions in humans, before progressing to human clinical trials.

Supporting information

S1 Table

Filled in ARRIVE guidelines checklist.



We wish to thank the veterinary nurses and technicians in the porcine intensive care facility, Department of Animal Science, Aarhus University for superb work with the animals.

Department of Vascular Surgery, Viborg Hospital and especially the scrub nurses for excellent help and assistance with the surgical equipment and procedures.

Laboratory assistant Inger Marie Jepsen, Department of Animal Science, Aarhus University for help and guidance with blood sample analyses.

Department of Animal Science, Aarhus University, Department of Clinical Microbiology, Odense University Hospital, and Department of Cancer and inflammation research, University of Southern Denmark (run by Associate Professor Karsten Skjødt) for the accessibility of laboratory facilities.

PhD René dePont Christensen, Research Unit of General Practice, University of Southern Denmark for statistical help and advice.

Postdoctoral fellow Joseph Ross, Department of Biochemistry and Molecular Biology, University of Southern Denmark for proofreading and revisions on English grammar and style.

Funding Statement

The study was financially supported by grants form the Research Council at Odense University Hospital received by MS, TEA, JKK, HJK, JSL (no grant number; and the Danish Heart Foundation (grant number: 14-R97-A5266; received by MS. The funders had no role in study design, data collection and analysis, decision to publish, or preparation of the manuscript.

Data Availability

Data Availability

Data files are held in a public repository and available at or DOI: 10.6084/m9.figshare.4643893.


1. Mussa FF, Hedayati N, Zhou W, El-Sayed HF, Kougias P, Darouiche RO, et al. Prevention and treatment of aortic graft infection. Expert Rev Anti Infect Ther. 2007;5(2):305–15. Epub 2007/04/04. doi: 10.1586/14787210.5.2.305 [PubMed]
2. Perera GB, Fujitani RM, Kubaska SM. Aortic graft infection: update on management and treatment options. Vasc Endovascular Surg. 2006;40(1):1–10. Epub 2006/02/04. doi: 10.1177/153857440604000101 [PubMed]
3. Swain TW 3rd, Calligaro KD, Dougherty MD. Management of infected aortic prosthetic grafts. Vasc Endovascular Surg. 2004;38(1):75–82. Epub 2004/02/05. doi: 10.1177/153857440403800110 [PubMed]
4. Bandyk DF. Antibiotics-why so many and when should we use them? Semin Vasc Surg. 2002;15(4):268–74. Epub 2002/12/13. doi: 10.1053/svas.2002.36262 [PubMed]
5. Chambers ST. Diagnosis and management of staphylococcal infections of vascular grafts and stents. Intern Med J. 2005;35 Suppl 2:S72–8. Epub 2005/11/08. [PubMed]
6. O'Connor S, Andrew P, Batt M, Becquemin JP. A systematic review and meta-analysis of treatments for aortic graft infection. J Vasc Surg. 2006;44(1):38–45. Epub 2006/07/11. doi: 10.1016/j.jvs.2006.02.053 [PubMed]
7. Lawrence PF. Conservative treatment of aortic graft infection. Semin Vasc Surg. 2011;24(4):199–204. Epub 2012/01/11. doi: 10.1053/j.semvascsurg.2011.10.014 [PubMed]
8. Roy D, Grove DI. Efficacy of long-term antibiotic suppressive therapy in proven or suspected infected abdominal aortic grafts. J Infect. 2000;40(2):184–7. Epub 2000/06/07. [PubMed]
9. Saleem BR, Meerwaldt R, Tielliu IF, Verhoeven EL, van den Dungen JJ, Zeebregts CJ. Conservative treatment of vascular prosthetic graft infection is associated with high mortality. Am J Surg. 2010;200(1):47–52. Epub 2010/01/16. doi: 10.1016/j.amjsurg.2009.05.018 [PubMed]
10. Yeager RA, Porter JM. The case against the conservative nonresectional management of infected prosthetic grafts. Adv Surg. 1996;29:33–9. Epub 1996/01/01. [PubMed]
11. Fux CA, Wilson S, Stoodley P. Detachment characteristics and oxacillin resistance of Staphyloccocus aureus biofilm emboli in an in vitro catheter infection model. J Bacteriol. 2004;186(14):4486–91. Epub 2004/07/03. PubMed Central PMCID: PMCPMC438612. doi: 10.1128/JB.186.14.4486-4491.2004 [PMC free article] [PubMed]
12. Hoiby N, Bjarnsholt T, Givskov M, Molin S, Ciofu O. Antibiotic resistance of bacterial biofilms. International journal of antimicrobial agents. 2010;35(4):322–32. Epub 2010/02/13. doi: 10.1016/j.ijantimicag.2009.12.011 [PubMed]
13. Klitgaard JK, Skov MN, Kallipolitis BH, Kolmos HJ. Reversal of methicillin resistance in Staphylococcus aureus by thioridazine. JAntimicrobChemother. 2008;62(6):1215–21. [PubMed]
14. Kristiansen MM, Leandro C, Ordway D, Martins M, Viveiros M, Pacheco T, et al. Phenothiazines alter resistance of methicillin-resistant strains of Staphylococcus aureus (MRSA) to oxacillin in vitro. IntJAntimicrobAgents. 2003;22(3):250–3. [PubMed]
15. Kristiansen MM, Leandro C, Ordway D, Martins M, Viveiros M, Pacheco T, et al. Thioridazine reduces resistance of methicillin-resistant staphylococcus aureus by inhibiting a reserpine-sensitive efflux pump. In Vivo. 2006;20(3):361–6. [PubMed]
16. Poulsen MO, Jacobsen K, Thorsing M, Kristensen NR, Clasen J, Lillebaek EM, et al. Thioridazine potentiates the effect of a beta-lactam antibiotic against Staphylococcus aureus independently of mecA expression. Research in microbiology. 2013;164(2):181–8. Epub 2012/10/24. doi: 10.1016/j.resmic.2012.10.007 [PubMed]
17. Poulsen MO, Scholer L, Nielsen A, Skov MN, Kolmos HJ, Kallipolitis BH, et al. Combination of thioridazine and dicloxacillin combats Methicillin-resistant Staphylococcus aureus infections in Caenorhabditis elegans. Journal of medical microbiology. 2014. Epub 2014/06/11. [PubMed]
18. Stenger M, Hendel K, Bollen P, Licht PB, Kolmos HJ, Klitgaard JK. Assessments of Thioridazine as a Helper Compound to Dicloxacillin against Methicillin-Resistant Staphylococcus aureus: In Vivo Trials in a Mouse Peritonitis Model. PloS one. 2015;10(8):e0135571 Epub 2015/08/13. doi: 10.1371/journal.pone.0135571 [PMC free article] [PubMed]
19. Hahn BL, Sohnle PG. Effect of thioridazine on experimental cutaneous staphylococcal infections. In Vivo. 2014;28(1):33–8. Epub 2014/01/16. [PMC free article] [PubMed]
20. Bonde M, Hojland DH, Kolmos HJ, Kallipolitis BH, Klitgaard JK. Thioridazine affects transcription of genes involved in cell wall biosynthesis in methicillin-resistant Staphylococcus aureus. FEMS microbiology letters. 2011;318(2):168–76. Epub 2011/03/08. doi: 10.1111/j.1574-6968.2011.02255.x [PubMed]
21. Thorsing M, Klitgaard JK, Atilano ML, Skov MN, Kolmos HJ, Filipe SR, et al. Thioridazine induces major changes in global gene expression and cell wall composition in methicillin-resistant Staphylococcus aureus USA300. PloS one. 2013;8(5):e64518 Epub 2013/05/22. PubMed Central PMCID: PMCPMC3656896. doi: 10.1371/journal.pone.0064518 [PMC free article] [PubMed]
22. Kvist M, Hancock V, Klemm P. Inactivation of efflux pumps abolishes bacterial biofilm formation. Applied and environmental microbiology. 2008;74(23):7376–82. Epub 2008/10/07. PubMed Central PMCID: PMCPmc2592912. doi: 10.1128/AEM.01310-08 [PMC free article] [PubMed]
23. Stenger M, Klein K, Gronnemose RB, Klitgaard JK, Kolmos HJ, Lindholt JS, et al. Co-release of dicloxacillin and thioridazine from catheter material containing an interpenetrating polymer network for inhibiting device-associated Staphylococcus aureus infection. Journal of controlled release: official journal of the Controlled Release Society. 2016;241:125–34. Epub 2016/09/25. [PubMed]
24. Dicillin® hårde kapsler 250 mg og 500 mg Sandoz A/S: Danish Medicines Agency; 2015. Available from:
25. Gao H, Lund L, Prag J, Sandermann J, Lindholt JS. Laparoscopic diagnosis and treatment of aortic vascular prosthetic graft infections in a porcine model. European journal of vascular and endovascular surgery: the official journal of the European Society for Vascular Surgery. 2008;35(1):41–5. Epub 2007/08/28. [PubMed]
26. Gao H, Sandermann J, Prag J, Lund L, Lindholt JS. Prevention of primary vascular graft infection with silver-coated polyester graft in a porcine model. European journal of vascular and endovascular surgery: the official journal of the European Society for Vascular Surgery. 2010;39(4):472–7. Epub 2010/01/12. [PubMed]
27. Gao H, Sandermann J, Prag J, Lund L, Lindholt JS. Rifampicin-soaked silver polyester versus expanded polytetrafluoro-ethylene grafts for in situ replacement of infected grafts in a porcine randomised controlled trial. European journal of vascular and endovascular surgery: the official journal of the European Society for Vascular Surgery. 2012;43(5):582–7. Epub 2012/03/17. [PubMed]
28. Robertshaw D. Dukes' Physiology of Domestic Animals: Cornell University; 2004
29. Medscape. thioridazine (Rx)—Mellaril 2015 [cited 2015 27th of July]. Available from:
30. Christensen JB, Hendricks O, Chaki S, Mukherjee S, Das A, Pal TK, et al. A comparative analysis of in vitro and in vivo efficacies of the enantiomers of thioridazine and its racemate. PloS one. 2013;8(3):e57493 Epub 2013/03/19. PubMed Central PMCID: PMCPMC3591432. doi: 10.1371/journal.pone.0057493 [PMC free article] [PubMed]
31. Dasgupta A, Mukherjee S, Chaki S, Dastidar SG, Hendricks O, Christensen JB, et al. Thioridazine protects the mouse from a virulent infection by Salmonella enterica serovar Typhimurium 74. International journal of antimicrobial agents. 2010;35(2):174–6. Epub 2009/12/17. doi: 10.1016/j.ijantimicag.2009.09.027 [PubMed]
32. Kristiansen JE, Sebbesen O, Frimodt-Moller N, Aaes-Jorgensen T, Hvidberg EF. Synergy between a non-neuroleptic thioxanthene stereo-isomer and penicillin in vivo. APMIS. 1988;96(12):1079–84. [PubMed]
33. Martins M, Viveiros M, Kristiansen JE, Molnar J, Amaral L. The curative activity of thioridazine on mice infected with Mycobacterium tuberculosis. In Vivo. 2007;21(5):771–5. [PubMed]
34. Harry DD. A Comparative Assessment of the Pig, Mouse and Human Genomes The Minipig in Biomedical Research: CRC Press; 2011. p. 323–42.
35. Daniel WA, Wojcikowski J. The role of lysosomes in the cellular distribution of thioridazine and potential drug interactions. Toxicology and applied pharmacology. 1999;158(2):115–24. Epub 1999/07/17. doi: 10.1006/taap.1999.8688 [PubMed]
36. Martins M, Bleiss W, Marko A, Ordway D, Viveiros M, Leandro C, et al. Clinical concentrations of thioridazine enhance the killing of intracellular methicillin-resistant Staphylococcus aureus: an in vivo, ex vivo and electron microscopy study. In Vivo. 2004;18(6):787–94. [PubMed]
37. Jortani SA, Valentour JC, Poklis A. Thioridazine enantiomers in human tissues. Forensic Sci Int. 1994;64(2–3):165–70. Epub 1994/02/01. [PubMed]
38. Pottegard A, Henriksen DP, Madsen KG, Hellfritzsch M, Damkier P, Stage TB. Change in International Normalized Ratio Among Patients Treated With Dicloxacillin and Vitamin K Antagonists. Jama. 2015;314(3):296–7. Epub 2015/07/22. doi: 10.1001/jama.2015.6669 [PubMed]
39. Yasuda K, Ranade A, Venkataramanan R, Strom S, Chupka J, Ekins S, et al. A comprehensive in vitro and in silico analysis of antibiotics that activate pregnane X receptor and induce CYP3A4 in liver and intestine. Drug metabolism and disposition: the biological fate of chemicals. 2008;36(8):1689–97. Epub 2008/05/29. [PMC free article] [PubMed]
40. Wojcikowski J, Maurel P, Daniel WA. Characterization of human cytochrome p450 enzymes involved in the metabolism of the piperidine-type phenothiazine neuroleptic thioridazine. Drug metabolism and disposition: the biological fate of chemicals. 2006;34(3):471–6. Epub 2005/11/08. [PubMed]
41. Thorn HA, Lundahl A, Schrickx JA, Dickinson PA, Lennernas H. Drug metabolism of CYP3A4, CYP2C9 and CYP2D6 substrates in pigs and humans. Eur J Pharm Sci. 2011;43(3):89–98. Epub 2011/03/31. doi: 10.1016/j.ejps.2011.03.008 [PubMed]
42. Niedzwiecki DM, Mailman RB, Cubeddu LX. Greater potency of mesoridazine and sulforidazine compared with the parent compound, thioridazine, on striatal dopamine autoreceptors. The Journal of pharmacology and experimental therapeutics. 1984;228(3):636–9. Epub 1984/03/01. [PubMed]
43. Jensen AS, Pennisi CP, Sevcencu C, Christensen JB, Kristiansen JE, Struijk JJ. Differential effects of thioridazine enantiomers on action potential duration in rabbit papillary muscle. European journal of pharmacology. 2015;747:7–12. Epub 2014/12/03. doi: 10.1016/j.ejphar.2014.11.015 [PubMed]
44. Ejim L, Farha MA, Falconer SB, Wildenhain J, Coombes BK, Tyers M, et al. Combinations of antibiotics and nonantibiotic drugs enhance antimicrobial efficacy. Nature chemical biology. 2011;7(6):348–50. Epub 2011/04/26. doi: 10.1038/nchembio.559 [PubMed]
45. Sabatini S, Gosetto F, Iraci N, Barreca ML, Massari S, Sancineto L, et al. Re-evolution of the 2-phenylquinolines: ligand-based design, synthesis, and biological evaluation of a potent new class of Staphylococcus aureus NorA efflux pump inhibitors to combat antimicrobial resistance. Journal of medicinal chemistry. 2013;56(12):4975–89. Epub 2013/05/29. doi: 10.1021/jm400262a [PubMed]
46. Fukumoto A, Kim YP, Hanaki H, Shiomi K, Tomoda H, Omura S. Cyslabdan, a new potentiator of imipenem activity against methicillin-resistant Staphylococcus aureus, produced by Streptomyces sp. K04-0144. II. Biological activities. J Antibiot (Tokyo). 2008;61(1):7–10. Epub 2008/02/29. [PubMed]
47. Koyama N, Tokura Y, Munch D, Sahl HG, Schneider T, Shibagaki Y, et al. The nonantibiotic small molecule cyslabdan enhances the potency of beta-lactams against MRSA by inhibiting pentaglycine interpeptide bridge synthesis. PloS one. 2012;7(11):e48981 Epub 2012/11/21. doi: 10.1371/journal.pone.0048981 [PMC free article] [PubMed]

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