Altered fecal microbiota composition in the Flinders sensitive line rat model of depression
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The gut microbiota is increasingly recognized as a potential mediator of psychiatric diseases. Depressed patients have been shown to have a different microbiota composition compared with healthy controls, and several lines of research now aim to restore this dysbiosis. To develop novel treatments, preclinical models may provide novel mechanistic insights.
Objective and methods
We characterized the gut microbiota of male adult Flinders sensitive line (FSL) rats, an animal model of depression, and their controls, Flinders resistant line (FRL) rats using 16S rRNA amplicon sequencing. Moreover, we performed fecal microbiota transplantation (using saline or pooled FRL/FSL feces) to study if the potential strain-specific differences could be transferred from one strain to the other, and if these differences were reflected in their depressive-like behavior in the forced swim test.
FSL rats tended to have lower bacterial richness and altered relative abundances of several bacterial phyla, families, and species, including higher Proteobacteria and lower Elusimicrobia and Saccharibacteria. There was a clear separation between FRL and FSL rat strains, but no effect of treatment, i.e., the bacterial composition of FSL rats receiving FRL feces was still more similar to FSL and not FRL rats. Similarly, the transplantation did not reverse behavioral differences in the forced swim test, although FSL feces significantly increased immobility compared with saline.
Our study showed that the gut microbiota composition of the depressive-like rats markedly differed from their controls, which may be of value for future microbiota-targeted work in this and similar animal models.
KeywordsDepression Gut-brain axis Fecal microbiota transplantation 16S rRNA amplicon sequencing
Fecal microbiota transplantation
Flinders resistant line
Flinders sensitive line
The gut microbiota is known to be involved in key physiological processes such as nutrient absorption, digestion, and metabolism. In addition to its homeostatic role, accumulating evidence suggests a widespread impact on human health and disease far beyond the gastrointestinal tract (Sekirov et al. 2010). These functions range from immune modulation to the development of distant tissues such as the bone, muscle, and brain, likely through bidirectional connections between the gut and extraintestinal organs (Fung et al. 2017). To exploit these communication systems for the benefit of human health, numerous studies in the past few decades have studied the effects of functional food supplements (e.g., prebiotics, probiotics, and synbiotics) and fecal microbiota transplantation (FMT).
Among many other observed health benefits, pre- and probiotics also positively affected mood and stress hormone concentrations in animals and healthy volunteers (Wallace and Milev, 2017, Wang et al. 2016, Dinan et al. 2013, Huang et al. 2016). In depressed patients, Akkasheh et al. (2015) found lower Beck Depression Inventory total scores after 8 weeks of probiotic supplementation, while Romijn et al. (2017) did not find evidence for antidepressant effects or changes in inflammatory markers. These studies differed in bacterial strain selection as well as disease severity and chronicity of the patient sample, which might explain conflicting results. Moreover, treatment response may have been affected by microbial group differences at baseline, as bacterial communities vary considerably according to the mode of delivery, host genetics, diet, health status, etc. (Rodriguez et al. 2015). In depressed patients, Jiang et al. (2015) found profound interindividual differences in alpha diversity according to treatment response and depression severity. Compared with healthy controls, depressed patients had decreased bacterial richness and diversity (Kelly et al. 2016). At the phylum level, they had increased relative abundances of Actinobacteria (Zheng et al. 2016, Jiang et al. 2015) and Proteobacteria (Jiang et al. 2015), and decreased Firmicutes (Jiang et al. 2015). Both increased (Jiang et al. 2015) and decreased (Zheng et al. 2016) levels of Bacteroidetes have been reported. Depressed patients also showed an increase in the order Bacteroidales and a decrease in the family Lachnospiraceae (Naseribafrouei et al. 2014). It is unknown whether these gut microbial changes reflect clinical symptoms and whether they are a cause or a result of the disease. Animal studies provided evidence to both, as stress caused gut microbial changes (O’Mahony et al. 2011, Bangsgaard Bendtsen et al. 2012, Abautret-Daly et al. 2018), Bailey et al. 2011) and gut microbiota transplantation from depressed patients induced depressive-like behavior in germ-free mice (Zheng et al. 2016) and microbiota-depleted rats (Kelly et al. 2016). These effects may be specific to microbiota-depleted models or human-derived feces, but they clearly demonstrate a causal association between gut microbiota and depressive-like behavior. To further explore this relationship, more data on conventional animals raised in non-sterile environments are needed.
Flinders sensitive line (FSL) rats show several behavioral and structural abnormalities compared with their control strain, Flinders resistant line (FRL) rats, and are used as an experimental animal model of depression (Overstreet and Wegener, 2013). Two recent studies in FSL rats found that probiotics protected against the pro-depressive-like effect of high-fat diet (Abildgaard et al. 2017) and induced changes in methyl donors and catecholamines (Tillmann et al. 2018). Given these data, further investigation of the gut-brain axis in these animals is of interest. To our knowledge, it is unknown if the gut microbiota composition of FSL rats differs from FRL controls, and how potential differences compare to depressed patients. However, this information may be useful in order to study causal mechanisms and to further investigate the gut-brain axis as a potential therapeutic target for depression. Our main objective was therefore to characterize the bacterial community of FSL vs. FRL rats using 16S rRNA amplicon sequencing to analyze whether their behavioral phenotype is related to potential differences in their gut microbiota composition. In addition, we performed FMT to investigate if potential microbial differences could be transplanted from one strain to the other and if these differences were reflected in their depressive-like behavior.
Materials and methods
Age-matched adult male Flinders sensitive line (FSL, n = 24) and Flinders resistant line (FRL, n = 24) rats were obtained from the breeding colony maintained at Aarhus University, Denmark. The day before the first transplantation, rats weighed 327.8 ± 40.7 g (mean ± SD) and were 10.6 ± 1.1 weeks old. Rats of the same strain and treatment were pair-housed in standard cages (Cage 1291H Eurostandard Type III H, 425 × 266 × 185 mm, Tecniplast, Italy) at 20 ± 2 °C and 60 ± 5% relative humidity on a reversed 12-h light/dark cycle (lights on at 2 p.m.). The reversed cycle was introduced in 3-h increments right before a 2-week acclimatization phase. After the acclimatization phase, rats were weighed once a week. All rats received standard chow diet (#1324 Altromin, Brogaarden, Lynge, Denmark) and tap water ad libitum and had access to a tunnel shelter, nesting material, and a wooden stick. Cages were changed once a week by the same experimenter performing the oral gavage and behavioral procedures. All experiments were approved by the Danish Animal Experiments Inspectorate prior to initiation of the experiments (approval number: 2012-15-2934-00254) and were conducted in accordance with the European Communities Council Directive.
Fecal material preparation
The day before the first transplantation, fresh fecal pellets were taken from the rectal ampulla of the rats and kept on wet ice immediately following collection. Feces from individual FRL rats were pooled to increase diversity and sample volume (the pool is hereafter referred to as “FRL feces”). Individual FSL fecal pellets were also pooled accordingly (“FSL feces”). Fecal material was prepared according to the European Consensus Conference for FMT in clinical practice (Cammarota et al. 2017), which was adapted for our study. The guidelines recommend 30 g of donor feces per person and transplantation to be diluted with sterile saline with 3–5 times larger volume of solvent (e.g., 30 g of feces diluted in 150 mL of saline). Assuming an average human weight of 70 kg, this is equivalent to 0.43-g feces per kg bodyweight. Accordingly, a 350-g rat should receive 0.15-g feces diluted in 0.75 mL saline. Our fecal collection yielded approximately 25 g of fecal material per pool, which was homogenized in 125 mL saline using a standard commercial blender. Before freezing at − 80 °C, 85% glycerol (Sigma-Aldrich, Steinheim, Germany) was added to a final concentration of 10% as per guideline recommendations. To avoid multiple freeze-thaw cycles, six aliquots per FRL/FSL pool for the six planned transplantations were prepared. On transplantation days, the designated aliquots were thawed in a warm (37 °C) water bath over 2 h immediately prior to transplantation. Rats were administered 0.75 mL fecal suspension per transplantation (consisting of 0.15 g pooled feces) using oral gavage.
Fecal pellets were collected on day 17 prior to behavioral testing and immediately frozen at − 80 °C. DNA was extracted using QIAamp PowerFecal DNA Kit (including a bead-beating step; #12830-50; Qiagen, Germany) according to the manufacturer’s instructions and sent to DNASense (Aalborg, Denmark) for 16S rRNA amplicon sequencing.
Bacterial V4 16S sequencing libraries were prepared using a custom protocol based on an Illumina protocol (#15044223 Rev. B, Illumina, San Diego, CA, USA). Up to 10 ng of extracted DNA was used as a template for PCR amplification of the 16S gene fragments. Each PCR reaction (25 μL) contained dNTPs (100 μM of each), MgSO4 (1.5 mM), Platinum® Taq DNA polymerase HF (1 U), 1× Platinum® High Fidelity buffer (Thermo Fisher Scientific, Oakwood, OH, USA), and tailed primer mix (400 nM of each forward and reverse). PCR was run with the following program: initial denaturation at 95 °C for 2 min, 35 cycles of amplification (95 °C for 20 s, 50 °C for 30 s, 72 °C for 60 s), and a final elongation at 72 °C for 5 min. Duplicate PCR reactions were performed for each sample and the duplicates were pooled after PCR. The forward and reverse tailed primers were designed according to the Illumina protocol (#15044223 Rev. B, 2015) and contained primers targeting the bacteria and archaea 16S gene V4 region (Caporaso et al. 2011): 5′-GTGCCAGCMGCCGCGGTAA (515F) and 5′-GGACTACHVGGGTWTCTAAT (806R). The primer tails enable attachment of Illumina Nextera adaptors for sequencing in a subsequent PCR. The resulting amplicon libraries were purified using the standard protocol for Agencourt Ampure XP Bead (Beckman Coulter, Brea, CA, USA) with a modified bead-to-sample ratio of 4:5. The DNA was eluted in 33 μL of nuclease-free water (Qiagen, Hilden, Germany). DNA concentration was measured using Qubit™ HS DNA Assay kit (Thermo Fisher Scientific, USA). Sequencing libraries were prepared from the purified amplicon libraries using a second PCR. Each PCR reaction (25 μL) contained 1× PCRBIO HiFi buffer (PCR Biosystems, London, UK), PCRBIO HiFi Polymerase (1 U) (PCR Biosystems, UK), adapter mix (400 nM of each forward and reverse), and up to 10 ng of amplicon library template. PCR was run with the following program: initial denaturation at 95 °C for 2 min, 8 cycles of amplification (95 °C for 20 s, 55 °C for 30 s, 72 °C for 60 s) and a final elongation at 72 °C for 5 min. The resulting sequencing libraries were purified using the standard protocol for Agencourt Ampure XP Bead (Beckman Coulter, USA) with a modified bead-to-sample ratio of 4:5. The DNA was eluted in 33 μL of nuclease-free water (Qiagen, Germany). DNA concentration was measured using Qubit™ HS DNA Assay kit (Thermo Fisher Scientific, USA). Gel electrophoresis using Tapestation 2200 and D1000 screentapes (Agilent, Lexington, MA, USA) was used to check the product size and purity of a subset of sequencing libraries. Double-indexing was performed on the libraries.
The purified sequencing libraries were pooled in equimolar concentrations and diluted to 2 nM. The samples were sequenced (2 × 301 bp) on a MiSeq (Illumina, USA) using a MiSeq Reagent Kit v3 (Illumina, USA) following the standard guidelines for preparing and loading samples on the MiSeq. To overcome low complexity issue often observed with amplicon samples, 20% Phix control library was spiked in.
Demultiplexing was done by the MiSeq software. Forward and reverse reads were trimmed for quality using Trimmomatic v. 0.32 (Bolger et al. 2014) with the settings SLIDINGWINDOW:5:3 and MINLEN:250. The trimmed forward and reverse reads were merged using FLASH v. 1.2.7 (Magoc and Salzberg, 2011) with the settings -m 10 -M 200. The merged reads were dereplicated and formatted for use in the UPARSE workflow (Edgar, 2013). Chimeras were removed as a de novo step in the UPARSE pipeline by default. The dereplicated reads were clustered using the usearch v. 7.0.1090 -cluster_otus command with default settings. Operational taxonomic unit (OTU) abundances were estimated using the usearch v. 7.0.1090 -usearch_global command with -id 0.97. Taxonomy was assigned using the RDP classifier (Wang et al. 2007) as implemented in the parallel_assign_taxonomy_rdp.py script in QIIME (Caporaso et al. 2011), using the MiDAS database v.1.23 (McIlroy et al. 2015). The results were analyzed in R through the Rstudio IDE using the ampvis package v.2.2.6 (Albertsen et al. 2015). Rarefaction curves were checked and showed a very low diversity community with the expected flattening curves (Supplementary Fig. 1).
All behavioral tests were performed in specially equipped rooms within the animal facility between 08:00 a.m. and 12:30 p.m. in the active phase of the animal under dim red light. The order of animals was determined randomly. To minimize stress, animals were habituated to the behavioral rooms 1 h before testing commenced. All arenas/tanks were thoroughly cleaned between each trial. Tests were scored by an observer blinded to strain and treatment groups.
To measure locomotion, rats were placed in an open-field arena (100 × 100 × 80 cm) immediately prior to the forced swim test as described previously (Tillmann et al. 2017). Briefly, animals were placed in the center of the square and allowed to move freely for 5 min, which was recorded by a camera mounted to the ceiling. The total distance traveled (cm) was obtained with specialized software tracking the midpoint of the rats’ body contour (Ethovision XT, Noldus Information Technology, Wageningen, Netherlands).
Forced swim test
To measure depressive-like behavior, the forced swim test (28) was employed as described previously (Tillmann et al. 2017). Briefly, rats were placed into a perspex cylinder (height, 60 cm; diameter, 24 cm) filled with 24 (± 1)°C heated tap water for 5 min. A camera was positioned in front of the water tanks to record their behavior. Three distinct behaviors were scored, including struggling (vertical movements of the forepaws), swimming (horizontal movements), and immobility (floating posture with minimal movements), whereby immobility was interpreted as depressive-like behavior (Slattery and Cryan, 2012).
Bodyweight and behavioral data were analyzed by a two-way ANOVA (strain × treatment). In case of a statistically significant treatment effect or interaction, these were followed up by the Bonferroni-corrected comparisons. Assumptions of normality and homogeneity of variances were tested by the Shapiro-Wilk test and Levene’s test, respectively. Data in the figures are presented as means ± standard error of the mean (SEM). Alpha was set at 0.05, while a p value between 0.05 and 0.1 was interpreted as a trend. Statistical analyses were carried out using IBM SPSS 22.0 (IBM Corp., Armonk, NY, USA). Graphs were generated using SPSS and GraphPad Prism 5.0 (GraphPad Software Inc., San Diego, CA, USA).
Relative abundances (log-transformed) at the phylum and family level were analyzed by mixed model regression: rat identity comprised the random effect (intercept), whereas fixed effects included rat strain, treatment, phylum/family, and their interactions. To investigate any associations with depressive-like behavior, the animals were divided into quartiles based on immobility in the forced swim test, and the forced swim test quartile was included in the model. Families/phyla not observed in > 50% of animals were excluded. Restricted maximum likelihood (REML) estimation was used, and residuals were considered independent by phylum/family. Contrasts of marginal linear predictions were used to test for differences between groups. The results are expressed as relative abundances with 95% CI, and analyses were performed with and without the Bonferroni correction as stated. Mixed model regression was performed with Stata 14 (StataCorp LT, TX, USA). At the OTU level, differential abundance was analyzed by DESeq2 (differential expression analysis based on the negative binomial distribution), and p values were adjusted by false discovery rate (FDR) according to Benjamini and Hochberg (Benjamini and Hochberg, 1995). In addition, the overall microbiota composition was analyzed by a principal component analysis (PCA) and a partial least-squares discriminant analysis (PLS-DA) with pareto scaling of the OTUs and a missing value tolerance of 50% with Simca 14 (MKS Umetrics AB, Sweden). The relationship between the first component (PC1) of the PLS-DA analysis and immobility behavior of the two strains was assessed by Spearman’s rank correlation.
Body weight and water/food intake
FSL rats weighed significantly less than FRL rats at both baseline (day 0; means ± SD, 301.6 ± 28.2 g vs. 354.0 ± 34.1 g; F(1,42) = 32.97, p < 0.001) and endpoint (day 17; 340.0 ± 27.1 g vs. 397.7 ± 34.6 g; F(1,42) = 39.51, p < 0.001), which is characteristic for their depressive-like phenotype (Overstreet, 1993). Treatment groups did not differ in body weight at baseline or endpoint (p’s > 0.355), and there was no interaction between strain and treatment (p’s > 0.676). There were no significant differences in water or food intake (grams of food per 100 g body weight) between strains or treatment groups (p’s > 0.181).
Gut microbiota analysis
DNA extraction was successful and yielded similar DNA concentrations for most samples (57.8 ± 3.5 ng/μL). Sample preparation for bacterial sequencing (V4) was also successful for all samples and yielded between 11,954 and 172,082 reads after quality control and bioinformatic processing. One sample (strain: FRL, treatment: saline) was unsuccessful and excluded from the microbiota results. All OTUs are provided in Supplementary Table 1.
Reduced gut microbiota richness in FSL rats
Multivariate inference revealed a clear separation between FSL and FRL rats
Phylum-level differences between strains and treatment groups
Two interactions between strain and treatment were observed before the Bonferroni correction was applied. In the Deferribacteres phylum (interaction, χ2 = 6.03; p = 0.049), treatment did not affect FSL rats (χ2 = 5.74; p = 0.28 (Bonferroni)), whereas a higher abundance was seen in FRL rats receiving FRL feces than in FRL rats receiving saline (0.01% (0.01–0.03) vs. 0.06% (0.03–0.12); z = 3.09; p = 0.006 (Bonferroni)). The second interaction was found in the Cyanobacteria phylum (interaction χ2 = 9.34; p = 0.009), but no follow-up tests reached statistical significance, although FSL feces treatment tended to cause lower Cyanobacteria abundance in FRL rats than in FSL rats (FRL receiving FSL feces, 0.40% (0.15–1.08); FSL receiving FSL feces, 0.07% (0.02–0.20); χ2 = 5.64; p = 0.09 (Bonferroni)). Treatment alone was not found to affect the microbiota composition at the phylum level. There were no main or interaction effects in Firmicutes:Bacteroidetes or Actinobacteria:Proteobacteria ratios (p’s > 0.330).
Family-level differences between strains and treatment groups
FSLs had a significantly higher abundance of Bifidobacteriaceae (0.05% (0.03–0.10) vs. 0.02% (0.01–0.03); χ2 = 11.5; p = 0.0007), but a lower abundance of Rikenellaceae (0.81% (0.62–1.06) vs. 1.87% (1.42–2.45); χ2 = 18.6; p < 0.0001), Elusimicrobiaceae (0.08% (0.05–0.13) vs. 0.26% (0.16–0.44); χ2 = 10.8; p = 0.001), Christensenellaceae (0.09% (0.07–0.13) vs. 0.28% (0.20–0.40); χ2 = 17.5; p < 0.0001), and Peptostreptococcaceae (0.01% (0.00–0.01) vs. 0.03% (0.02–0.05); χ2 = 19.3; p < 0.000) than FRL rats. All these alterations remained statistically significant after the Bonferroni correction (p’s < 0.037).
Without the Bonferroni correction, FSLs also had a lower abundance of Bacteroidales S24-7 group (2.74% (2.15–3.50) vs. 4.44% (3.46–5.69); χ2 = 4.62; p = 0.03), Peptococcaceae (0.03% (0.02–0.04) vs. 0.04% (0.03–0.06); χ2 = 4.55; p = 0.03), and Eubacteriaceae (0.001% (0.001–0.002) vs. 0.002% (0.002–0.003); χ2 = 3.91; p = 0.048), but a higher abundance of Lactobacillaceae (3.38% (2.66–4.29) vs. 2.79% (2.19–3.56); χ2 = 3.99; p = 0.046), Lachnospiraceae (9.58% (7.69–11.94) vs. 7.92% (6.32–9.91); χ2 = 5.85; p = 0.02), Veillonellaceae (2.06% (1.39–3.04) vs. 0.94% (0.63–1.40); χ2 = 8.98; p = 0.003), and Helicobacteraceae (1.37% (1.01–1.85) vs. 0.76% (0.56–1.03); χ2 = 7.00; p = 0.008).
Treatment affected several microbial families. A marked treatment effect was seen for Rhodospirillaceae (χ2 = 20.4; p < 0.0001). Specifically, FRL feces-treated rats had a higher abundance than saline-treated rats (0.15% (0.08–0.30) vs. 0.02% (0.01–0.05); z = 4.51; p < 0.001 (Bonferroni)), and the same was the case for treatment with FSL feces (0.07% (0.03–0.13); z = 2.53; p = 0.03 (Bonferroni)). However, FSL and FRL feces groups did not differ (z = 1.83; p = 0.2 (Bonferroni)). In addition, three other families were affected by treatment, although these changes did not remain statistically significant after the Bonferroni correction: For Bifidobacteriaceae (χ2 = 7.56; p = 0.02), FRL feces led to a higher abundance than saline (0.05% (0.02–0.10) vs. 0.02% (0.01–0.04); z = 2.52; p = 0.04 (Bonferroni)), whereas the effect of FSL feces narrowly missed significance in comparison with saline (0.04% (0.02–0.08); z = 2.36; p = 0.06 (Bonferroni)). FSL and FRL feces groups did not differ (z = 0.00; p = 1.0). For Deferribacteraceae (χ2 = 10.5; p = 0.005), treatment with FRL feces caused higher levels than treatment with FSL feces or saline (saline, 0.02% (0.01–0.04); FRL feces, 0.06% (0.04–0.10); FSL feces, 0.03% (0.02–0.05); p’s < 0.02 (Bonferroni)). Similarly, FRL feces caused higher abundance of Peptostreptococcaceae (χ2 = 8.23; p = 0.02) compared with FSL feces and saline (saline, 0.01% (0.00–0.02); FRL feces, 0.03% (0.01–0.05); FSL feces, 0.01% (0.00–0.02); p’s < 0.05 (Bonferroni)).
A single treatment × strain interaction was found for OTUs belonging to unclassified families (χ2 = 9.67; p = 0.008), but only before the Bonferroni correction was applied. Specifically, FSL feces led to different abundancies in the two strains (FRLs receiving FSL feces, 2.20% (1.54–3.15) vs. FSLs receiving FSL feces, 0.83% (0.56–1.23); χ2 = 12.8; p = 0.002 (Bonferroni)).
OTU-level differences between FRL and FSL
Since the PLS-DA analysis revealed a clear effect of strain on the gut microbiota composition, we also compared FRL rats with FSL rats on the lowest taxonomic level, the OTU level. In total, 475 OTUs were detected, and 167 (35%) of these were found to differ between the rat strains after statistical correction (Supplementary Table 2). Most of the significantly different OTUs were found at a higher level in FRL rats (109), whereas only 58 were found at a higher level in FSL rats.
Among the significantly different OTUs between FSL and FRL rats, FSLs had lower relative abundances of all 15 OTUs from the Bacteroidales S24-7 family, all four OTUs from the Candidatus Saccharimonas genus, both OTUs from the Alistipes genus, and both OTUs from the Roseburia genus.
FSL rats had higher abundances of all six OTUs from the Blautia genus and all four OTUs from the Subdoligranulum genus. Of the three significantly different OTUs from the Lactobacillus genus, two were found in lower relative abundances in FSL rats and one in higher abundance. There was no significant difference in Bifidobacteria.
Fecal transplantation altered behavior in the forced swim test
In the forced swim test, FSL rats struggled significantly less than FRL rats (128 ± 28 s vs. 154 ± 40 s; F(1,42) = 8.03, p = 0.007, Fig. 6b) and were more immobile (96.3 ± 48.6 s vs. 56.7 ± 44.7 s; F(1,42) = 9.51, p = 0.004, Fig. 6d). The strains did not differ in their total swimming duration (p = 0.213, Fig. 6c). There were significant treatment effects in struggling (F(2,42) = 3.88, p = 0.028) and immobility (F(2,42) = 4.05, p = 0.025). Bonferroni multiple comparisons of the treatment groups revealed that rats receiving FRL feces struggled less than saline-treated ones (p = 0.041), while there was no difference between FSL feces and saline or FSL and FRL feces (p’s > 0.098). There was a trend towards a strain × treatment interaction in struggling (F(2,42) = 2.84, p = 0.070). FSL feces administration significantly increased immobility compared with saline (p = 0.023), whereas FRL feces did not differ from saline (p = 0.224). There was no difference in immobility between FSL and FRL feces (p = 1.00).
Associations between gut microbiota composition and behavior
To explore whether the behavioral difference between FSLs and FRLs may be linked to their gut microbial composition, we analyzed the relationship between immobility and the first component (PC1) of the PLS-DA analysis, since this component represented the composite microbial pattern that ultimately separates the two strains. However, no correlation was evident between PC1 and FRL immobility scores (r = 0.034, n = 23, p = 0.877) or FSL immobility scores (r = 0.103, n = 24, p = 0.631).
In addition, we examined correlations between immobility and the 20 individual OTUs that were best at separating FSL and FRL rats, but found no significant effect (data not shown).
We also divided the animals into quartiles based on their immobility duration and analyzed their relationship with phylum and family abundancies in the mixed regression model. At the phylum level, no significant associations were seen between quartile of immobility and microbial abundancies. At the family level, however, Alcaligenaceae abundance decreased with increasing immobility levels (Q1, 0.39% (0.28–0.55); Q2, 0.28% (0.23–0.34); Q3, 0.20% (0.16–0.24); Q4, 0.14% (0.10–0.20); z = −3.41; p = 0.02 (Bonferroni)).
Our findings demonstrate that the gut microbiota composition of the depressive-like FSL rats significantly differed from control FRL rats. FSL rats had not only a tendency to a lower number of OTUs but also altered relative abundances of several phylum-, family-, and species-level bacteria. Fecal transplantation with pooled FSL or FRL feces did not reverse these bacterial differences. On a behavioral level, FSL feces significantly increased immobility in the forced swim test compared with saline but not compared with FRL feces.
Microbial richness and diversity
Lower bacterial richness as observed in FSL rats was also found in depressed patients compared with healthy controls (Kelly et al. 2016). However, it must be noted that the richness difference in our study was largely driven by elevated levels in FRL rats receiving pooled feces rather than saline, suggesting that treatment-naïve FSL and FRL rats may not differ in bacterial richness. A lack of difference in species richness between depressed patients and controls was also found in several human studies (Naseribafrouei et al. 2014, Jiang et al. 2015). We found no evidence for altered alpha diversity levels between FSL and FRL rats, and human data are inconclusive in that regard, with studies reporting both increased (Jiang et al. 2015), decreased (Kelly et al. 2016), or similar (Naseribafrouei et al. 2014) diversity in depressed vs. non-depressed participants. Conflicting studies may be due to heterogeneous patient or control groups, analytical methods, confounding medication, diet, or a combination thereof. Data on microbial richness and diversity in animal models of depression are sparse, but a recent study in mice reported reduced richness and diversity following social defeat (Bharwani et al. 2016). Galley et al. (2014) further noted that restraint stress in mice caused reduced alpha diversity in colonic mucosa- but not luminal-associated communities, whereas richness was not reduced in either microbial niche. Park et al. (2013) demonstrated that experimentally induced depression in mice through olfactory bulbectomy changed the composition of the microbiota, but the authors did not assess richness or diversity.
Gut microbiota composition in FSL vs. FRL rats
We were able to differentiate FSL from FRL rats on the basis of their gut microbiota using PLS-DA analysis (R2(Y) = 0.8; Q2 = 0.7). When fecal transplantation treatment groups were included as identifiers, the predictive value decreased substantially (R2(Y) = 0.1; Q2 = 0.05), indicating that the model was able to predict rat strain but not treatment. Similarly, we found several strain differences between FSL and FRL rats on phylum, family, and species levels, but only limited effects of treatment. On the phylum level, FSL rats had significantly lower relative abundances of Elusimicrobia and Saccharibacteria than FRLs. Before the Bonferroni correction, FSLs had higher abundances of Proteobacteria. Interestingly, Jiang et al. (2015) corroborated this finding in depressed patients, suggesting that the overrepresentation of Proteobacteria may be associated with depression. A recent review further noted that these gram-negative bacteria are often increased in intestinal and extraintestinal diseases with an inflammatory phenotype, and that they may serve as a potential diagnostic marker of dysbiosis and risk of disease (Rizzatti et al. 2017). Given the close connection between depression and inflammation (Miller and Raison, 2016), future causal studies of the relationship between Proteobacteria and depression are warranted.
On the family level, FSLs had a lower relative abundance of Rikenellaceae, Elusimicrobiaceae, Christensenellaceae, and Peptostreptococcaceae. Before the Bonferroni correction, they also had lower abundances of Bacteroidales S24-7 group, Peptococcaceae, and Eubacteriaceae. Interestingly, Rikenellaceae has previously been associated with fear (Christian et al. 2015) and depression (Jiang et al. 2015) in humans, and its member Alistipes was found to be increased in stress-exposed mice (Bangsgaard Bendtsen et al. 2012), indicating that this family may be involved with psychiatric symptomatology. Bacteroidales S24-7 group was found to be reduced in mice following restrained stress (Wong et al. 2016). FSLs had higher relative abundances of Bifidobacteriaceae and, before Bonferroni correction, Lactobacillaceae, Lachnospiraceae, Veillonellaceae, and Helicobacteraceae. In mice, Lachnospiraceae was found to be increased following restraint stress (Wong et al. 2016), whereas human studies reported lower relative abundances in depressed patients compared with healthy controls (Jiang et al. 2015, Naseribafrouei et al. 2014).
At the OTU level, FSL rats had lower relative abundances of the genera Candidatus Saccharimonas, Alistipes, and Roseburia. Previous work showed that mice treated with 5-fluorouracil, a model of intestinal mucositis, had decreased abundances of Candidatus Saccharimonas (Li et al. 2017), which may be indicative of intestinal dysbiosis in FSL rats. The Alistipes genus has previously been found to be overrepresented in depressed patients (Naseribafrouei et al. 2014, Jiang et al. 2015), which is in contrast to our findings in the depressed rat model. Several species of the Roseburia genus have been suggested as a marker of health due to their butyrate-producing properties (Tamanai-Shacoori et al. 2017). Butyrate is one of the three major short-chain fatty acids and is generally associated with positive effects on health (Canani et al. 2011). An underrepresentation of Roseburia in FSL rats may thus be indicative of decreased butyrate production, and this should be explored by future studies. FSLs had higher relative abundances of Blautia and Subdoligranulum genera. The Blautia genus was found to be overrepresented in depressed patients compared to controls (Jiang et al. 2015), which is in line with our findings. Two of the three significantly different OTUs from the Lactobacillus genus were found in lower abundances in FSL rats, whereas one was found in higher abundances compared to FRL rats. Lactobacilli are usually associated with health benefits and a depletion may be correlated to a depressive-like phenotype (Marin et al. 2017, Aizawa et al. 2016). Bifidobacteria also generally exert health-promoting effects (O’Callaghan and van Sinderen, 2016), but we did not find any significant differences in FSL vs. FRL rats.
Effects of fecal transplantation on gut microbiota and behavior
Fecal transplantation from FSL to FRL rats and vice versa did not appear to shift the strain-characteristic phyla- and family-level differences; for instance, the increased relative abundance of Proteobacteria found in FSL rats did not decrease upon transplantation with FRL feces. Interestingly, Elusimicrobia/Elusimicrobiaceae seemed to be increased in FRL rats receiving FSL feces, but not in FSL rats, although both received the same pooled fecal suspension, and although these bacteria were only present in FSL rats in low abundances. Similar observations can be made for Saccharibacteria. FSL feces also lowered the abundance of Cyanobacteria in FRL but not FSL rats. FRL rats may therefore be more receptive to the introduction of these bacteria, but the functional consequences remain elusive. Administration of FRL feces caused a higher relative abundance of several bacterial families, such as Rhodospirillaceae, Bifidobacteriaceae, Deferribacteraceae, and Peptostreptococcaceae. Increased abundance of bacteria upon the introduction of feces independent of the origin would perhaps not be surprising, but the distinct strain-dependent increase in FRL feces compared with FSL feces warrants further investigation.
Behavioral analyses confirmed the depressive-like phenotype of FSL rats in the forced swim test, in that FSLs were more immobile and struggled less than FRL rats (Overstreet and Wegener, 2013). Transplantation with FSL feces increased immobility, supporting a transmissible behavioral phenotype. However, the effect was only significant compared with saline and not compared with FRL feces, limiting the overall generalizability of this finding. Contrary to our initial hypothesis, transplantation with FRL feces did not decrease immobility in FSL rats. According to our microbiota analyses, the identified characteristic bacteria for the strains were not transmissed, which might explain the limited behavioral effect. Zheng et al. (2016) found alterations in the forced swim test following FMT from depressed patients to germ-free mice. In contrast, although Kelly et al. (2016) we are able to shift the bacterial composition in microbiota-depleted rats following FMT from depressed patients, they did not observe concurrent behavioral changes in the forced swim test, implying that some neurobiological correlates of depression may not be transmissible through FMT. Other potentially relevant behavioral tests (i.e., anhedonia, cognition, and anxiety) were not conducted in the present study because FSL and FRL rats do not usually differ in these domains (Overstreet and Wegener, 2013, Tillmann et al. 2018), and a behavioral transmission from one strain to another would therefore not be of immediate interest. Fecal treatment in general seemed to decrease struggling in FRL rats compared with saline, again suggesting that FRL rats may be more susceptive to the introduction of certain bacteria and hence may possess a more malleable microbiota than FSLs. However, since feces contain significant amounts of non-bacterial matter (e.g., colonocytes, archaea, viruses, fungi, protists, and metabolites (Bojanova and Bordenstein, 2016)), the effects of the bacterial transplant alone cannot be separated, and conclusions should be drawn with caution.
To further investigate if the behavioral difference between FSL and FRL rats may be linked to their gut microbiota, we correlated immobility to the first component of the PLS-DA analysis, the component that ultimately separated the two strains. We also correlated immobility to the 20 individual OTUs that were best at separating the strains, but found no effects. Interestingly, Alcaligenaceae abundance decreased with increasing immobility levels, i.e., animals that were more immobile had a lower relative abundance of the bacteria. Alcaligenaceae was previously found to be increased in sedentary rats selectively bred for low-capacity running (Panasevich et al. 2016) as well as rats on a high-fat diet (Khan et al. 2018), suggesting a metabolic component which may also be relevant to consider in case of the forced swim test given the difference in energy effort between immobile and struggling rats. This family has also been positively associated with cognitive decline in cirrhosis patients (Bajaj et al. 2012), i.e., lower abundance reflected better memory.
Strengths and limitations
While our study has significant strengths such as the use of non-sterile animals, an additional non-fecal control group, and long-term FMT treatment, several limitations should be mentioned. Our FMT protocol was based on the human consensus guidelines (Cammarota et al. 2017) and on previous attempts in rodents (Mell et al. 2015, Bercik et al. 2011, Bruce-Keller et al. 2015), but limited data from rats raised in non-sterile environments are available. Thus, several other experimental parameters could be explored by future studies, such as amount and preparation of feces or frequency and duration of treatments, which may improve the transmissibility of the strain-characteristic bacteria. Another limitation of the present study is the fact that FMT was not performed in anaerobic conditions, which may cause the loss of anaerobic strains. Moreover, our results cannot be generalized to FSL/FRL rats of a different age or gender, as these factors may change the microbial composition (Rodriguez et al. 2015, Haro et al. 2016). Microbial abundances also vary considerably between species, and the sparsity of studies within the gut-brain axis in rats with intact microbiota further complicates comparisons to previous work. However, rats raised in non-sterile environments may provide a more translational approach compared with, e.g., germ-free mice. Furthermore, rats were proposed to be more representative of the human gut microbiota than mice (Nguyen et al. 2015, Wos-Oxley et al. 2012), highlighting the importance of investigating the effects of FMT in rats rather than mice. Despite greater similarities between rat and human microbiota, the diversity of the rat intestinal microbiome was found to be 2–3 times higher than in humans, which may be due to a higher complexity in the rat gut bacterial ecosystem to harvest more nutrient from the basic laboratory diet (Manichanh et al. 2010). Thus, it is unknown if our results are comparable to a clinical population. We chose not to administer antibiotics prior to transplantation, as previous studies have shown that the establishment of donor phylotypes is not increased by prior antibiotic depletion (Manichanh et al. 2010). However, other studies have found behavioral and metabolic results following antibiotic treatment (Kelly et al. 2016), and we cannot exclude that microbiota depletion may have exerted differential effects in the present study. It was assumed that by performing repetitive gavage for several days, the gut microbiome community and structure would have reached its final equilibrium. As no longitudinal data were obtained during the FMT, we cannot conclude whether not observing differences in the gut microbiome of the different treatments was due to not starting with a low abundance microbiome, not performing the FMT long enough, or because there were indeed no differences. To reduce the number of animals used in this study, we used the same animals as donors and recipients, and, as a consequence, we transplanted fecal pellets. While the cecum may resemble the gut microbiota more closely, transplanting and analyzing feces may hold more translational value to humans. Finally, only recipient feces were analyzed in the present study, but the additional analysis of donor feces may provide additional mechanistic insights in future studies.
This is the first study characterizing the gut microbiota community in FSL and FRL rats and transplanting a potentially strain-specific microbial profile from one rat strain to another. We found several rat strain differences in their bacterial profile, and some of these differences were comparable to those found in depressed patients (e.g., the increase in Proteobacteria and Blautia), while others are novel findings. The fecal transplant did not shift the profile towards the transplanted strain (i.e., FSL rats receiving FRL feces still had a more similar behavioral and microbial profile to FSL and not FRL rats). Fecal administration independent of the donor strain seemed to generally decrease mobility in the forced swim test compared to saline, whereas mobility in the OF was not affected. Future studies should investigate other animal models of depression and the consequences of FMT on behavior and microbiota. Moreover, the functional role of strain-characteristic microbiota should be elucidated in more detail.
Compliance with ethical standards
All experiments were approved by the Danish Animal Experiments Inspectorate prior to initiation of the experiments (approval number: 2012-15-2934-00254) and were conducted in accordance with the European Communities Council Directive.
Conflict of interest
Gregers Wegener reported having received lecture/consultancy fees from H. Lundbeck A/S, Servier SA, AstraZeneca AB, Eli Lilly A/S, Sun Pharma Pty Ltd., Pfizer, Inc., Shire A/S, HB Pharma A/S, Arla Foods Amba., Janssen Pharma A/S., and Mundipharma International, Ltd. All other authors report no potential conflicts of interest.
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