[Retracted] Correlations between Intestinal Microbiota and Clinical Characteristics in Colorectal Adenoma/Carcinoma

Participants were from outpatients who received the colonoscopy at the First Affiliated Hospital, Zhejiang University School of Medicine. All colorectal adenoma patients and colorectal cancer patients had not undergone endoscopic or surgical treatment. Exclusion criteria included patients older than 90 years of age, patients with a personal history of colorectal cancer, colorectal adenoma, and inflammatory bowel disease or a family history of colorectal cancer, and patients who had used antibiotics within two months or received chemotherapy/radiation treatments within six months. Colonoscopy was performed by experienced endoscopists. Written informed consent was obtained from all participants. From June 2020 to December 2020, fresh fecal samples (≥1 g) were collected from all participants before colonoscopy and immediately frozen at -80°C until further processing for 16S rRNA gene sequencing analysis. The clinical characteristics of the patients were recorded, including age, sex, tumor size, location, TNM stage, differentiation degree, pathological pattern, and histology. Unfortunately, we were not able to recruit healthy controls in the First Affiliated Hospital, Zhejiang University School of Medicine. Therefore, the corresponding data of control (n = 199) was obtained from the Kesic Dataset of a project for predicting the age based on the gut microbiota (https://www.kesci.com/home/project/5ddb6bedf41512002cebd995↗). The study protocol was approved by the Medical Ethics Committee of the First Affiliated Hospital, Zhejiang University School of Medicine (2017-869). In addition, all patients signed informed consent forms.

Total genomic DNA extraction from fecal samples was performed using a QIAamp DNA Stool Mini Kit (QIAGEN, Germany) following the manufacturer's instructions. The quality and concentration of DNA were verified with 2% agarose gel (Tanon, China) and a NanoDrop spectrophotometer (Thermo Fisher Scientific, USA).

High-throughput Illumina sequencing of the V3-V4 variable regions of the 16S rRNA gene was performed using universal primers 343F (5′-TACGGRAGGCAGCAG-3′) and 798R (5′-AGGGTATCTAATCCT-3′). The PCR reaction was carried out with 15 μL of Phusion® High-Fidelity PCR Master Mix (New England Biolabs, United States), 0.2 μM of forward and reverse primers, and about 10 ng template DNA. Thermal cycling consisted of initial denaturation at 98°C for 1 min, followed by 30 cycles of denaturation at 98°C for 10 s, annealing at 50°C for 30 s, and elongation at 72°C for 30 s followed by a final extension of 5 min at 72°C.

The amplicon was purified with AMPure XP beads (Beckman Coulter, USA) and subjected to a secondary PCR reaction. The final amplicon was quantified using a Qubit dsDNA assay kit (Life Technologies, USA). A sequencing library was generated using the TruSeq® DNA PCR-Free Sample Preparation Kit (Illumina, USA) following the manufacturer's recommendations and assessed on the Qubit^@ 2.0 Fluorometer (Thermo Fisher Scientific, USA) and Agilent Bioanalyzer 2100 system (Agilent Technologies, USA). The library was sequenced on an Illumina NovaSeq platform, and 250 bp paired-end reads were generated.

The FASTQ files were processed using QIIME (V1.9.1, http://qiime.org/scripts/split_libraries_fastq.html↗). Paired-end reads were merged using FLASH (V1.2.7, http://ccb.jhu.edu/software/FLASH/↗). Quality filtering on the raw tags was performed under specific filtering conditions to obtain high-quality clean tags. The effective tags were obtained by detected chimera sequences, and the chimera sequences were removed using the UCHIME algorithm (UCHIME algorithm version 10.0, http://www.drive5.com/usearch/manual/uchime_algo.html↗) based on the reference database (SILVA database version 123, https://www.arb-silva.de/↗). Sequences with 97% sequence homology were assigned to the same operational taxonomic units (OTUs) by using UPARSE software (version 7.0.1001, http://www.drive5.com/uparse/↗). The representative sequence for each OTU was screened for further annotation. All representative reads were annotated and blasted against the SILVA database (version 123, http://www.arb-silva.de/↗) using the RDP classifier (confidence threshold was 70%). OTU abundance information was normalized using a standard of sequence number corresponding to the sample with the least sequences.

Alpha diversity and beta diversity analyses were performed by using QIIME (version 1.9.1). Alpha diversity was applied in analyzing complexity of species diversity for samples. The community richness and diversity were described by the Chao index and Shannon index, respectively. Beta diversity analysis was used to evaluate comparisons between groups among samples and assessed by nonmetric multidimensional scaling (NMDS) analysis and principal coordinate analysis (PCoA) by using a weighted UniFrac distance matrix. Linear discriminant analysis (LDA) effect size [12] was used to identify differentially abundant bacterial taxa associated with groups of participants. The LDA value threshold was set at 4. The t-test and Wilcox test were employed to assess the significance by using QIIME (version 1.9.0).

A total of 373 participants, including 154 CRC patients (mean age of 65.81 ± 10.98 years, 63.64% male), 20 AD patients (mean age of 64.35 ± 12.89 years, 75.00% male), and 199 healthy controls (mean age of 59.48 ± 3.20 years, 58.29% male), were enrolled in this study. The clinical characteristics of the patients are shown in Table 1. The mean size of carcinoma was 4.55 ± 2.18 mm, and most of the tumors were found in the left colon (75.97%). In the CRC group, the differentiation degree concentrated in the moderate degree (75.32%) and mainly tubular adenocarcinoma (85.06%).

A total of 2,668 OTUs were generated from 164 patients' samples. The Venn diagram showed that 1,323 OTUs were shared between AD and CRC, while 113 unique OTUs existed in AD and 1232 unique OTUs existed in CRC (Figure 1(a)). The rarefaction curve and species accumulation boxplot are shown in Figures 1(b) and 1(c). The value of Good's coverage for each group was over 99.8% (Figure 1(d)). No significant difference in alpha diversity was observed between AD and CRC groups (P = 0.95 for the Chao index, Figure 1(e); P = 0.74 for the Shannon index, Figure 1(f)). A mild separation between AD and CRC was observed, and no significant difference in microbiota composition was detected by PCoA (Pr(>F) = 0.33 for weighted UniFrac distance, Figure 1(g)). NMDS analysis also revealed that the microbiota composition between the two groups was similar; samples from AD and CRC mostly overlapped with one another (stress = 0.202 > 0.2, Figure 1(h)). The analysis of beta diversity revealed that fecal microbial communities between AD and CRC were not distinct from each other (P = 0.88 for weighted UniFrac distance, Figure 1(i)). However, there was more dispersion in control samples than in AD/CRC samples in both the PCoA and NMDS plots (stress = 0.123 < 0.2, Figures 1(j) and 1(k)), suggesting that the fecal microbial communities between control and AD/CRC were different.

The bacterial community from 154 CRC and 20 AD patients' fecal samples was classified into 28 phyla, 45 classes, 99 orders, 178 families, 423 genera, and 461 species. At the genus level, the intestinal microbiota was dominated by Bacteroides (30.75%), Prevotella (14.03%), and Faecalibacterium (5.51%) in control (Figure 2(a)). The dominant genera in CRC were Bacteroides (25.92%), Faecalibacterium (6.39%), and Fusobacterium (3.38%), while the dominant genera in AD were Bacteroides (25.92%), Faecalibacterium (6.39%), and Blautia (4.08%) (Figure 2(a)).

The significant analysis based on the Wilcox test showed that 115 genera of intestinal microbiota in AD patients were distinct from those in controls. Correspondingly, there were 134 genera significantly different in CRC patients compared with control (Figure 3(a)). Besides, there were 4 genera significantly different among the three groups, namely, Acidaminococcus, Alloprevotella, Mycoplasma, and Sphingobacterium (Figure 3(b)). Notably, the relative abundance of Acidaminococcus was decreased with the order of control-AD-CRC. LEfSe analysis was used to identify the specific taxa associated with CRC. Only one family (Prevotellaceae) is enriched in CRC (Figure 3(c)). Parvimonas, Peptostreptococcus, Prevotella, Butyricimonas, Alistipes, and Odoribacter were key genera in the network of colorectal adenoma/carcinoma-associated bacteria (Figure 3(d)). Furthermore, random forest analysis suggested that a combination of the top 10 species showed the best performance in distinguishing AD patients from CRC patients (AUC = 85.54%, 95% CI: 78.83%-92.25%, Figure 3(e)). Mean Decrease Gini (MDG) and Mean Decrease Accuracy (MDA) coefficients were used to rank the importance of the variables from random forest algorithm results (Figures 3(f) and 3(g)). The 10 most important species were Butyricimonas synergistica, Agrobacterium larrymoorei, Bacteroides plebeius, Lachnospiraceae bacterium feline oral taxon 001, Clostridium scindens, Prevotella heparinolytica, bacterium LD2013, Streptococcus mutans, Lachnospiraceae bacterium 19gly4, and Eubacterium hallii.

To explore the correlations between intestinal microbiota and clinical characteristics, we created the correlation heatmap according to the different clinicopathologic features of CRC patients. As shown in Figure 4(a), 154 patients were divided into two groups according to their age: 13 CRC patients were younger than 50 years old and 141 patients were older than 50 years old, and 15 bacterial species were higher and another 15 bacterial species were significantly lower in the old patients than in the young patients. Additionally, 1 phylum (Firmicutes, P < 0.05, data not shown) dramatically decreased in the old patients compared to the young patients. Stratified by sex, a heatmap was created to summarize the association between the microbiome and sex (Figure 4(b)), and 5 bacterial species increased in female patients including Prevotella sp. Marseille-P2931, Clostridium colinum, Bifidobacterium pseudocatenulatum, Gordonibacter sp. Marseille-P2775, and Saccharibacteria bacterium UB2523. The other 11 bacterial species are significantly enriched in male patients (Figure 4(b)). Figure 4(c) shows the association results stratified by tumor location. The microbiome was different between the patients with the tumor in the left and right colon, in which 17 bacterial species were found obviously changed (7 up and 10 down, left vs. right). Interestingly, the relative abundance of Bacteroides cellulosilyticus was significantly increased with the order of differentiation degree in poor-moderate-well (P < 0.05, data not shown). Furthermore, we compared the relationship between microbiota and tumor stages in CRC (I-II vs. III-IV). The relative abundances of 9 bacterial species, including Porphyromonas uenonis, Clostridium colinum, Proteiniphilum sp., Selenomonas ruminantium, Gordonibacter sp. Marseille-P2775, Akkermansia muciniphila, Rikenella microfusus, Dialister pneumosintes, and Weissella cibaria, were significantly higher in the TNM stage III/IV group than in the TNM stage I/II group (Figure 4(d)).

The data used to support the findings of this study are included within the article.