Molecular Testing for Gastrointestinal Cancer

Abstract

With recent advances in molecular diagnostic methods and targeted cancer therapies, several molecular tests have been recommended for gastric cancer (GC) and colorectal cancer (CRC). Microsatellite instability analysis of gastrointestinal cancers is performed to screen for Lynch syndrome, predict favorable prognosis, and screen patients for immunotherapy. The epidermal growth factor receptor (EGFR) tyrosine kinase inhibitor has been approved in metastatic CRCs with wildtype RAS (KRAS and NRAS exon 2–4). A BRAF mutation is required for predicting poor prognosis. Additionally, amplification of human epidermal growth factor receptor 2 (HER2) and MET is also associated with resistance to EGFR inhibitor in metastatic CRC patients. The BRAF V600E mutation is found in sporadic microsatellite unstable CRCs, and thus is helpful for ruling out Lynch syndrome. In addition, the KRAS mutation is a prognostic biomarker and the PIK3CA mutation is a molecular biomarker predicting response to phosphoinositide 3-kinase/AKT/mammalian target of rapamycin inhibitors and response to aspirin therapy in CRC patients. Additionally, HER2 testing should be performed in all recurrent or metastatic GCs. If the results of HER2 immunohistochemistry are equivocal, HER2 silver or fluorescence in situ hybridization testing are essential for confirmative determination of HER2 status. Epstein-Barr virus–positive GCs have distinct characteristics, including heavy lymphoid stroma, hypermethylation phenotype, and high expression of immune modulators. Recent advances in next-generation sequencing technologies enable us to examine various genetic alterations using a single test. Pathologists play a crucial role in ensuring reliable molecular testing and they should also take an integral role between molecular laboratories and clinicians.

Gastric cancer (GC) and colorectal cancer (CRC) are the most common malignancies originating from the gastrointestinal tract [1]. GC is the fourth most commonly diagnosed cancer, and CRC is the third most common cancer in men and the second most common in women worldwide [2]. According to the 2013 nationwide cancer statistics in South Korea, GC and CRC were the third and fourth leading causes of age-standardized cancer mortality [3], respectively, and 34,331 and 37,986 new cases of GC and CRC, respectively, are expected to occur in 2016 [4].

Major advances in molecular technologies during the past two decades have led to a better understanding of the pathogenesis and management of GCs and CRCs, in particular, adenocarcinomas. The discovery of microsatellite instability (MSI) in gastrointestinal cancers, especially in colorectal adenocarcinomas, has broadened our understanding of carcinogenesis and genetic susceptibility [5]. RAS mutation analysis results are critical for predicting resistance to epidermal growth factor receptor (EGFR) inhibitors in metastatic CRC patients, increasing the importance of molecular diagnosis in CRCs [6]. The detection of Epstein-Barr virus (EBV) by in situ hybridization (ISH) has enabled the identification of a distinctive subtype of GC [7], and the efficacy of trastuzumab therapy in GC has proven the clinical relevance of molecular testing in a treatment-related perspective [8]. In addition, trastuzumab therapy is approved in human epidermal growth factor receptor 2 (HER2)–positive advanced esophageal adenocarcinoma [8], but most genetic alterations reported in esophageal adenocarcinoma do not show significant differences compared to GC [1]. MSI testing is recommended in small intestinal adenocarcinoma [9], and KRAS and BRAF mutations are found in a subset of small intestinal adenocarcinoma [10]. However, the incidence of small intestinal adenocarcinoma is too low to review comprehensively.

In this article, we aim to review the current status of various molecular tests for gastrointestinal cancers in Korean patients, specifically gastric adenocarcinoma and colorectal adenocarcinoma considering their national disease burden, and suggest standardized methods and quality control measures. Furthermore, by reviewing the findings from the most recent studies on the molecular features of gastrointestinal cancers, we propose a future next-generation sequencing (NGS) panel for diagnostic, predictive, and prognostic purposes.

MOLECULAR TESTS

Microsatellite instability

Background

Microsatellites are short tandem DNA repeats that are randomly dispersed throughout the human genome, showing significant polymorphism between individuals. MSI is defined as a change in the microsatellite region within a tumor in comparison to that of normal tissue, resulting from either deletion or insertion of repeating units. MSI is caused by a defect in the DNA mismatch repair (MMR) mechanism which normally occurs during DNA replication to correct errors [11]. Since the early 1990s, it has been reported that a subset of CRC is microsatellite unstable (MSI-high frequency [MSI-H]), and that MSI represents a novel mechanism for colorectal carcinogenesis [12].

MSI is the hallmark genetic aberration of Lynch syndrome [11]. Lynch syndrome is currently diagnosed when a pathogenic germline mutation is identified in one of the DNA MMR genes, MLH1, PMS2, MSH2, MSH6, or MLH3, and accounts for 2%–4% of all CRCs. Families who meet the Amsterdam criteria for the diagnosis of Lynch syndrome are referred to as having hereditary nonpolyposis CRC [13]. Screening and diagnosis of Lynch syndrome in clinical practice are required in order to reduce various cancer-related risks in the families. Therefore, screening for Lynch syndrome is necessary in newly diagnosed CRC patients, especially in the young or those with family history. Screening is usually done with MSI analysis and immunohistochemistry (IHC) for the four MMR enzymes MLH1, PMS2, MSH2, and MSH6 [14]. Additionally, the loss of epithelial cell adhesion molecule (EpCAM) expression has been demonstrated in a small subset of Lynch-syndrome–associated CRCs, which is caused by germline EpCAM deletions [15,16]. In Lynch syndrome, the risk of extracolonic lesions is high including gastric, endometrial, renal pelvis/ureter, small bowel, ovarian, brain, hepatobiliary tract, and sebaceous cancers [1,17].

Sporadic MSI-H is observed in about 15%–20% of sporadic CRCs in Western countries and in about 5%–6% in Eastern countries and is caused by MLH1 promoter hypermethylation and MLH1 expression loss [11,18,19]. In sporadic CRC patients, MSI status is confirmed as a good prognostic marker [9,20,21]. CRCs with MSI-H frequently show high grade morphology, such as mucin production, signet ring cells, medullary features, and undifferentiated histology, but their biological behavior is less aggressive compared to that of microsatellite stable (MSS) or MSI-low frequency (MSI-L) CRCs [1]. MSI-H is observed in about 10% of sporadic GCs and is associated with older age, antral location, and intestinal type histology [22,23]. The independent prognostic value of MSI status in GC remains controversial; however, a recent meta-analysis showed that MSI-H is associated with better overall and disease-specific survival in GC [24]. Recent advances in genome analysis of CRCs and GCs showed that MSI-H is strongly associated with a distinct subtype characterized by elevated mutation rates (“hypermutated”) [25-27]. Cristescu et al. [27] demonstrated that MSI-H GCs have the best overall and disease-free survival among four molecular subtypes. The new American Joint Committee on Cancer (AJCC) cancer staging manual (8th edition) recommended obtaining the results of MSI testing additionally in both GC and CRC patients for clinical care [9].

It is generally accepted that a defective MMR system is associated with decreased therapeutic response to fluorouracil-based adjuvant chemotherapy in CRCs and GCs [28]. In contrast, Le et al. [29] demonstrated that MSI status in CRCs and non-CRCs (including gastric, endometrial, biliary, and small bowel cancers) is an excellent predictive factor for favorable treatment outcome by immune checkpoint blockade with pembrolizumab. Furthermore, high expression of checkpoint molecules, such as PD-1, PD-L1, CTLA-4, LAG-3, and IDO, is characteristic of gastrointestinal cancers with MSI-H phenotype [30-32], which suggests that MSI-H tumors are good candidates for immunotherapy.

Indication

Growing evidence has supported the rationale for universal MSI testing in CRC, which showed a higher sensitivity for identifying Lynch syndrome among newly diagnosed CRC [33]. Considering the significant clinical implications of MSI status from both treatment- and prognostic-related perspective, it is recommend that all patients with newly diagnosed GC or CRC be tested for MSI status. MSI testing can be performed in any advanced tumors for immune checkpoint inhibitor treatment.

Methodology

Methods

MSI analysis is performed by polymerase chain reaction (PCR) amplification of DNA extracted from both tumor and corresponding normal tissue, followed by separation of the amplified product by capillary gel electrophoresis. The results are determined by comparison of the peak patterns with a shift in PCR product size of the tumor compared to that of the normal tissue. Currently, the gold standard of MSI testing is the Bethesda panel [5], which uses PCR for the analysis of the fragment length of five markers: two mononucleotide repeats (BAT25 and BAT26) and three dinucleotide repeats (D5S346, D2S123, and D17S250). Recently developed MSI testing consists of a pentaplex panel of quasimonomorphic mononucleotides markers (NR-27, NR-21, NR-24, BAT-25, and BAT-26), which allows the analysis of MSI in tumors without the need of normal control (reference) DNA [34]. The sensitivity or limit of detection of MSI analysis is approximately 10%, but can vary according to laboratory conditions.

Confirming the loss of MMR proteins (MLH1, PMS2, MSH2, MSH6) by IHC should also be used for the screening of Lynch syndrome. Since PMS2 and MLH1 form a heterodimer, MLH1 loss is related to PMS2 loss observed by IHC. MSH6 forms a heterodimer with MSH2, thus MSH2 loss occurs with concurrent MSH6 loss. However, loss of PMS2 or MSH6 does not lead to loss of MLH1 or MSH2. When compared to PCR-based method, IHC is known to have sufficient sensitivity, specificity, and predictive values [35]. However, the resting expression level of MMR proteins is very low; thus, a reliable diagnosis requires an adequate amount (quantity) of tissue sample and pathologists’ experiences in daily practice. For the accurate interpretation of loss of MMR proteins in tumor tissue, internal positive controls such as adjacent non-neoplastic glands, lymphocytes, or stromal cells should show strong nuclear positivity. Longer cold ischemia time or under-fixation can cause false negative results.

Type of specimen

Both fresh frozen and formalin-fixed paraffin embedded (FFPE) tissues are considered suitable for PCR-based methods. Paired PCR results of cancer and matched normal tissues from the same patient are necessary for proper interpretation of the results.

Specimen requirements

Approximately 1 cm² of the tumor and normal tissues is required. Needless to state, the most important requirement of the specimen is a sufficient amount of DNA [36]; one of the most common reasons for false-negative MSI results is low tumor cellularity in the sample, for example, conditions such as mucinous carcinoma. Therefore, to ensure a sufficient proportion of the tumor cells, microdissection of the tumor cell area selected by experienced pathologists is generally recommended and widely implemented in many laboratories. Tumor cells should occupy at least 50%–60% of the examined tissue sections [37].

Reporting

In pathologic reports, patient information, such as patient ID, name, gender, and age, order date, ordering physician, and surgical pathologic diagnosis and number should be included. MSI tumors can be divided into three groups: MSI-H, when ≥ 30% of markers exhibit instability; MSI-L, when <30% of markers show instability; and MSS, when none of the markers exhibit instability (Fig. 1). According to the Bethesda panel, MSI-H is defined by having instability of two or more makers, MSI-L is defined by having instability of only one marker, and MSS means none of five markers show instability. The results of MSI must be reported as MSS, MSI-L, or MSI-H. Interpretation of the molecular diagnosis and signature of the pathologist are also required for the final diagnosis.

Fig. 1.

Fragment pattern of microsatellite instability–high case by GeneScan analysis.

Validation of test

MSI analysis should be validated in each pathology laboratory as laboratory-developed tests. Since the requirements for proper validation of MSI tests are not clearly defined, an external program checklist can be referred to for validation, including that of accuracy, precision, reportable range of the test results, analytic sensitivity and specificity, and positive and negative predictive values. It is recommended to directly compare the results of MSI tests to those of MMR protein IHC or MLH1 promoter hypermethylation testing.

Quality assurance

Each pathology laboratory should establish internal quality assurance (QA) instructions for MSI analysis and review all performed MSI tests in regular QA meetings. In each MSI test, specialized pathologists should confirm the examined tumor and normal area. Positive and negative controls should be used in each run of PCR and fragmentation analysis. Additionally, we recommend that both MSI tests and IHC for MMR proteins are performed and compared for reliable test results. All pathology laboratories should participate in external QA programs.

Somatic mutation analysis

Background

RAS mutations

The proto-oncogene KRAS encodes a GTPase, which is an early player in the EGFR induced RAS/RAF/mitogen-activated protein kinase (MAPK) signaling pathway. KRAS mutations have important roles in various aspects of carcinogenesis, and KRAS mutations in exon 2 at codons 12 and 13 have been reported to be detected in approximately 35%–45% of CRCs. Negative correlations between KRAS mutations and MSI or BRAF mutations suggest that these molecular alterations are associated with a distinct subset of CRCs and have prognostic significance [38]. MSI-H status is associated with a favorable prognosis [20,21], whereas many previous studies supported the association of KRAS mutation with a poor prognosis [39,40]. AJCC recommended obtaining the results of KRAS mutational testing in CRC patients for predicting patient prognosis [20], and the poor prognostic effect of KRAS mutation is also described in the new AJCC cancer staging manual (8th edition) [9].

Targeted therapies directed against EGFR tyrosine kinase have improved treatment efficacy and patients’ survival in various cancers, including CRCs [41]. EGFR blockers cetuximab and panitumumab have proven anti-tumor activity as monotherapies and in combination with chemotherapy and/or radiation in CRC patients [42,43], and EGFR signaling–associated genes have been studied for their relationship with responsiveness to EGFR inhibitors (Fig. 2). KRAS mutations in exon 2 at codons 12 and 13 are associated with resistance to cetuximab and panitumumab, and with poor survival in chemo-refractory metastatic CRC patients [44]. Additionally, oncogenic mutations in KRAS codons 59, 61, 117, and 146 and NRAS codons 12, 13, and 61 have been reported in approximately 3%–5% of CRC samples [45,46]. Recent clinical trials have demonstrated that extended RAS mutation testing, including that for mutations in KRAS and NRAS exons 2 to 4, can be more predictable for lack of responsiveness to EGFR inhibitors than previously proven KRAS exon 2 testing in first-line chemotherapy for metastatic CRC patients [6,47]. Recently, RAS mutation testing is approved as a companion diagnosis for EGFR inhibitor treatment in metastatic CRC patients.

Fig. 2.

Epidermal growth factor receptor (EGFR)–related signaling pathway in metastatic colorectal cancer. Anti-EGFR antibodies are able to block downstream signal of EGFR in wild type RAS and RAF (left), but unable to block in mutant RAS or RAF (right). mTOR, mammalian target of rapamycin; MAPK, mitogen-activated protein kinase.

BRAF mutations

The oncogenic BRAF mutation has a role in constitutive activation and downstream signaling along the MAPK signaling pathway. BRAF mutations occur in approximately 5%–8% of CRCs and most are the BRAF V600E mutation, however, the BRAF V600E mutation almost never occurs in GCs [48,49]. The BRAF mutation is an early molecular event in the serrated pathway of CRC. Molecular sequencing in serrated pathway CRCs has been reported as BRAF mutation/CpG island methylator phenotype (CIMP)/MSI-H or BRAF mutation/CIMP/MSS/p16 loss [50]. Many previous studies have confirmed that the BRAF mutation is associated with poor prognosis in metastatic CRC patients [6,47]. In addition to metastatic CRCs, earlier-stage CRC patients with mutated BRAF have been reported to show significantly worse overall survival than that of patients with wild-type BRAF [51,52]. Especially, this prognostic significance was evident in the MSS CRC group [9,52].

The BRAF V600E mutation is observed in approximately two thirds of microsatellite unstable CRCs caused by MLH1 hypermethylation and protein loss, but it never occurs in microsatellite unstable CRCs associated with Lynch syndrome [53]. Therefore, newly diagnosed CRC cases should be initially examined by MSI analysis with MMR protein IHC, and then Lynch syndrome can be excluded if both MLH1 loss by IHC and BRAF V600E mutation or MLH1 hypermethylation are observed. Further germline mutational analysis for diagnosing Lynch syndrome is commonly performed in patients with MLH1 loss by IHC and BRAF wild type or unmethylated MLH1 (Fig. 3).

Fig. 3.

Algorithm of molecular testing in colorectal cancer (CRC) patients. MSI, microsatellite instability; IHC, immunohistochemistry; MSI-H, microsatellite instability–high; MSS, microsatellite stable.

For targeted therapies directed against EGFR tyrosine kinase in metastatic CRC patients, oncogenic mutations related to the EGFR signaling pathway are also suggested to be clinically relevant. Theoretically, the BRAF V600E mutation is considered a negative predictive marker for response to EGFR tyrosine kinase inhibitors, and several studies have shown that BRAF V600E mutations were significantly predictable for resistance to single-agent EGFR inhibitor [54,55]. The predictive role of the BRAF V600E mutation remains inconclusive owing to its rare prevalence [6,47], but the level of evidence for the BRAF V600E mutation in CRC is I for blocking the effect of anti-EGFR antibody therapy according to the new AJCC cancer staging manual (8th edition) [9].

In contrast to BRAF mutated melanomas, the results of early clinical trials using BRAF inhibitors were not successful in treating BRAF mutated CRCs [56,57]. However, several clinical trials that combine BRAF and EGFR inhibitors with or without a third agent are currently ongoing or have recently been completed in BRAF mutated CRCs [58].

PIK3CA mutations

In addition to the RAS/RAF/MAPK signaling pathway, activated EGFR can also induce the phosphoinositide 3-kinase (PI3K)/AKT/PTEN pathway. PIK3CA mutations in exon 9 and 20 have been studied as effectors of the EGFR downstream signaling pathway, similar to BRAF and RAS, and they might be related to resistance to EGFR inhibitors [59]. However, PIK3CA mutations tend to occur together with KRAS mutations [54,60]. Furthermore, confirmative evidence for a role of PIK3CA mutations in predicting response to cetuximab has not been shown [61]. Therefore, the role of PIK3CA mutations in routine predictive molecular testing for EGFR inhibitor therapy remains controversial.

The PI3K/AKT/mammalian target of rapamycin (mTOR) pathway is frequently dysregulated in human cancers initiated by various molecular alterations including PIK3CA mutations. Janku et al. [62] performed early-phase clinical trials in which PI3K/AKT/mTOR inhibitors were administered to the patients with advanced tumors, and demonstrated that PIK3CA mutation was independently associated with a better response to PI3K/AKT/mTOR inhibitors.

Many previous studies have reported the prognostic implication of PIK3CA mutations in CRC; some studies have shown a significant correlation between PIK3CA mutations and patient survival, but other studies have not [63]. Although World Health Organization (WHO) classification suggests that PIK3CA mutations are markers for poor prognosis [1], its practical role for predicting a patient’s outcome remains uncertain.

Recently, experimental evidence suggests that cyclooxygenase 2 inhibition of aspirin down-regulates the PI3K signaling pathway. Liao et al. [64] reported that regular use of aspirin after cancer diagnosis in PIK3CA-mutated CRC patients was associated with a better prognosis [65], which suggests that PIK3CA mutations may serve as molecular biomarkers for predicting response to aspirin therapy.

Indication

Based on confirmative correlation with patient prognosis, KRAS mutation testing is recommended in all patients with newly diagnosed CRC. The results of BRAF mutation testing are required for predicting a patients’ prognosis in both metastatic and earlier stage CRC and for excluding Lynch syndrome in all CRC patients. Especially in metastatic CRC patients, KRAS and NRAS mutational analysis should be performed for predicting the responses to anti-EGFR antibody therapy, and BRAF mutations are essential as poor prognostic biomarkers. Although the prognostic or predictive role of PIK3CA mutation is not clear, molecular testing for PIK3CA mutation may be necessary for predicting response to PI3K/AKT/mTOR inhibitors and aspirin therapy after CRC diagnosis.

Methodology

Method

Sanger sequencing

Sanger sequencing is a traditional and well-confirmed method which needs ubiquitous instruments and inexpensive reagents, thus Sanger sequencing has been considered the gold standard method in many pathology laboratories for detecting oncogenic gene mutations [66]. In addition, Sanger sequencing has advantages for genetic mutational analysis such as the ability to identify specific mutations and to detect new mutations, and it has high reliability [66]. However, direct sequencing has some disadvantages including lower sensitivity (about 10%–20%), a multistep time-consuming method, subjective data interpretation, and no standardization [60]. Sequencing is not able to detect small amounts of mutated DNA fragments—especially less than 20% of total DNA—in the sample. Accordingly, the tumor samples should be very carefully prepared for to ensure collection of high tumor content.

Pyrosequencing

Compared to Sanger sequencing, pyrosequencing is more sensitive, and it can detect approximately 5% of mutant alleles [67]. It has some advantages compared to Sanger sequencing: (1) it is faster and more convenient; (2) the percentage of mutant allele quantity can be obtained; (3) it can be performed in a closed system in a single well; and (4) it can run multiple samples [68]. Therefore, this technology has provided sufficient analytical sensitivity and specificity for identifying KRAS, NRAS, and BRAF mutations in FFPE samples, even those from tissues with low tumor cell contents [69]. Pyrosequencing also has some disadvantages: (1) it requires additional costly instruments as compared to Sanger sequencer, as well as expensive reagents and consumables; (2) its data analysis is complex and challenging; (3) it can only sequence a short length of nucleotide sequence; and (4) it cannot detect new mutations [70]. However, the read length is sufficient for KRAS, NRAS, and BRAF sequencing because hot spots of these mutations are located within short length sequences.

Real-time PCR–based mutation detection methods

The detection of KRAS mutations using real-time PCR-based commercial kits has been suggested to be more reliable and sensitive than sequencing methods. The merits of commercial kits using real-time PCR systems are high sensitivity (approximately 1%), fast turn-around time, straightforward data interpretation, a closed-tube with a one-step process, small intra- and inter-lot deviations, and good concordance among the different real-time PCR systems. The disadvantages are that they have a relatively high cost per sample and high DNA input requirements [71]. In addition, they cannot detect all mutations or identify specific mutations.

The currently used commercial kits for detecting KRAS mutations are as follows: Asuragen, DxS TheraScreen KRAS mutation detection kit, EntroGen, Roche COBAS, TrimGen Mutector II KRAS kit, and ViennaLab [71]. Kim et al. [72] reported that KRAS mutational status was discordant between primary and metastatic sites in 17.5% of samples, using the Sanger sequencing method. In contrast, Miglio et al. [73] demonstrated concordant KRAS mutation status and type of mutation between primary and metastatic tumors and successful amplification in fine needle aspiration biopsy specimens with low tumor cell numbers, using the TheraScreen test. The TheraScreen KRAS RGQ PCR Kit uses Scorpions and ARMS technologies and detects six mutations in codon 12 and one in codon 13 of KRAS. The COBAS KRAS mutation test kit (Roche Molecular Systems, Inc., Branchburg, NJ, USA) is a TaqMelt PCR assay and can detect 19 KRAS mutations in codons 12, 13, and 61. The COBAS test was also reported to have higher sensitivity than Sanger sequencing and can detect minor mutations including G13C, G13R, and Q61H, which are detected in less than 1% of CRCs [60,74].

Another real-time PCR–based method, the peptide nucleic acid (PNA)–clamp assay, has recently been approved in Korea. The PNA-clamp assay utilizes PNAs that are modified DNA that recognize and bind to their complementary nucleic acid sequences with greater stability and specificity and cannot function as primers for DNA polymerases. PNA-clamp PCR is a low cost and highly sensitive method (0.1% of sensitivity) for detecting mutated genes, and is useful in clinical practice [75]. The PNA-clamp mutation detection kit cannot identify specific mutations.

For improving detection sensitivity, high-resolution melting analysis, mutant-enriched PCR (enriched PCR–restriction fragment length polymorphism assay), and co-amplification at lower denaturation temperature–PCR methods can be applied in clinical mutation tests [71].

Next-generation sequencing

As mentioned above, mutations in the genes related to the EGFR signaling network may be responsible for resistance to EGFR inhibitors or worse overall survival in CRC patients, but it is difficult and less practical to test all related gene mutations including KRAS exon 2–4, NRAS exon 2–4, BRAF V600E, and PIK3CA in each individual metastatic CRC patient using conventional methods. Therefore, a high-throughput method is more practical or recommended for sequencing multiple EGFR signaling-related genes in a single test to detect various mutations. Recently, several studies have demonstrated the advantages of NGS including high sensitivity and specificity compared to those of PCR-based commercial kits and sequencing methods [70,76]. The above testing methods are summarized in Table 1.

Table 1.

Comparison among various detection methods for gene mutation analysis

	Sanger sequencing	Pyrosequencing	Real-time PCR	PNA-clamp assay	Next generation sequencing
Advantage	Gold standard	More rapid and sensitive than Sanger sequencing	Simple and fast	Simple and fast	High-throughput
Instrument	Ubiquitous	Not ubiquitous	Depending on kit	Ubiquitous	Costly equipment
Sensitivity (%)	10–20	5	1	0.1	1
Method	Labor-intensive, time-consuming	Convenient, closed system	Closed system, one-step process	Closed system, one-step process	Time-consuming
Mutant allele quantity (%)	Unmeasurable	Measurable	Unmeasurable	Unmeasurable	Measurable
Detect all or new mutation	Yes	No	No	No	Yes
Detect specific mutation	Yes	Yes	No	No	Yes
Data interpretation	Subjective	Less subjective, but complex	Simple and easy	Simple and easy	Complicated (need statistics)

PCR, polymerase chain reaction; PNA, peptide nucleic acid.

Type of specimen

The sample can be fresh, frozen, or FFPE. Surgical resection, endoscopic or needle biopsies, and cytology specimens are all acceptable sample types for mutation tests. If possible, the resection specimen is recommended for molecular analysis. However, biopsies are more commonly provided in inoperable advanced and metastatic CRC patients, and moreover, only cytology specimens may be available. Therefore, in such cases, the detection method should be successful with low total DNA quantity and highly sensitive for samples with a low tumor to total DNA ratio.

Specimen requirements

The tissue specimen should contain cancer cells and a pathologist needs to estimate the content of tumor cells. Tumor cell enrichment by micro- or macro-dissection is required to increase the sensitivity of mutation tests. FFPE blocks are commonly available for mutation tests, but formalin fixation induces DNA denaturation and degradation [77]. Prolonged formalin fixation, decalcification, and prolonged storage of the paraffin blocks negatively affect the integrity of DNA [78], and the specimen quality is important for successful test results. The pathologist has the responsibility of selecting the most appropriate tissue block and tumor area to be tested.

Reporting

With patient and clinical information, the absence or presence of a gene mutation should be reported in the pathologic records. If possible, the affected codon and specific change should be indicated. Appropriate nomenclature should be used and ambiguous terms are not recommended in reports. The reports should also include specimen type and test method used.

Validation of test

The analytical performance of both sequencing and commercial kits should be validated in each laboratory. It is recommended at least 40 samples be tested with many days and runs [79]. Both samples with known and unknown mutational status are recommended for validation. Additional comparative methods may be done with each testing method. The results of the validation should be analyzed by assessing accuracy, precision, analytical sensitivity and specificity, reportable range, and reference range [79].

Quality assurance

Each pathology laboratory should establish internal QA instructions for using each mutation analysis method and review all performed mutation analysis in regular QA meetings. The sequence information of wild- and mutant-types and their clinical significance should be determined. Each PCR test should include positive and negative controls. The laboratory must compare test positivity rate to its reported range, and maintain testing trends including clinical implications of gene mutation, concordance between methods, and positivity rates. All pathology laboratories should participate in external QA programs.

Gene amplification and rearrangements

Background

Targeting of oncogenic drivers has been increasingly applied clinically in several advanced human malignancies resulting in improvement of overall survival. At this moment, a few receptor tyrosine kinase inhibitors, such as trastuzumab, ramucirumab, and cetuximab, have been approved for targeted therapy. In addition, EGFR family (HER1–4), fibroblast growth factor receptor 2 (FGFR2), and MET are being explored as potential therapeutics and some have been successful in early-stage trials.

HER2

HER2 has important oncogenic roles including modulation of cell growth, differentiation, and survival. Protein overexpression of HER2 mainly occurs through HER2 gene amplification, resulting in subsequent activation of abnormal cell signaling [80]. After the successful results of the Trastuzumab for Gastric Cancer (ToGA) trial [8], trastuzumab against HER2 has been approved for the treatment of HER2-positive advanced GC. HER2 testing is necessary in daily practice for treatment of advanced GC patients and the recommended HER2 testing algorithm is presented in Fig. 4.

Fig. 4.

Recommended gastric human epidermal growth factor receptor 2 (HER2) testing algorithm. IHC, immunohistochemistry.

Following the success of the ToGA trial, HER2 blockade has been of great clinical interest in CRC [81-83]. Somatic HER2 amplification occurs in approximately 2%–7% of metastatic colorectal adenocarcinomas [81-83], and HER2-positivity (IHC3+ or IHC2+/amplification) is observed in about 5% of advanced CRCs [83]. HER2 gene amplification has been reported to be more frequent in rectal cancer than in right or left colon cancer [82]. KRAS mutation and HER2 amplification were suggested to be mutually exclusive [84], but our previous study demonstrated that HER2 amplification might occur in KRAS-mutated CRCs [60]. A few clinical trials with trastuzumab-based combinations have been performed [83,85,86]. Although earlier studies reported controversial results [85], recent trials suggest the possibility of HER2 blockade as a targeted therapy in advanced CRC patients [84]. Together, the HERACLES and MyPathway trials supported preclinical results that targeting HER2 with trastuzumab plus either lapatinib or pertuzumab is more effective than standard combination chemotherapy in HER2-positive CRC patients [83,86].

For predicting response to EGFR inhibitors such as cetuximab, RAS mutation has been approved as a companion diagnosis. In addition to RAS mutation, gene amplification of the receptor tyrosine kinases HER2 has been shown to bypass EGFR signaling and activate the MEK-ERK cascade, suggesting predictive roles of this gene. This has been supported by a previous study that identified HER2 amplification in samples from metastatic CRC patients who did not benefit from EGFR inhibitor treatment [87].

FGFR2

Clinical trials using antibodies against FGFR2b are now being conducted in GC patients. Oncogenic activation of FGFR2 via gene amplification occurs in a subset of common cancers, especially diffuse type GC [88,89]. FGFR2 amplification has been detected in about 8% of gastroesophageal cancers [88]. AZD4547 is a selective FGFR1–3 inhibitor with activity in FGFR2 amplified cancer models. In the SHINE trial in advanced GC patients with FGFR2 amplification or polysomy, AZD4547 was well-tolerated, but there was no progression-free survival benefit in the AZD-treated group [90]. However, in a recent translational clinical trial, GCs with high-level clonal FGFR2 amplification have a high response rate to the selective FGFR2 inhibitor AZD4547 [91].

MET and others

In addition to HER2 amplification, MET amplification was also found in a small subset of RAS and BRAF wild-type metastatic patients and is suggested to be associated with resistance to cetuximab treatment [92]. MET exon 14 deletion has been postulated to be one potential mechanism for MET protein overexpression [93]. A recent study suggested MET amplification as a novel mechanism of the resistance to EGFR and BRAF combination blockade in BRAF-mutated CRCs; furthermore, the study showed that switching from EGFR to MET inhibition resulted in clinical response of the disease [94].

KRAS gene amplification is observed in a minor subset of CRC cases (1%–2%) and has been reported to be nearly always mutually exclusive with KRAS mutations [45]. The database by the The Cancer Genome Atlas (TCGA) network has shown that NRAS, BRAF, and CRAF gene amplification can also be observed in a very low prevalence (<1%), but their clinical implication is not clear [26].

ROS1 gene rearrangement

ATP-binding sites in the kinase domains of anaplastic lymphoma kinase (ALK) and ROS1 share 77% amino acid identity [95]. In vitro evidence suggests that ROS1 may be a more sensitive target than ALK to inhibition by crizotinib [96]. The incidence of ROS1 rearrangement in gastric adenocarcinomas has been reported to be between 0.5% and 1% [95,97].

NTRK gene rearrangements

Neurotrophic tropomyosin receptor kinase (NTRK) gene rearrangements have oncogenic and transforming potential, and recently have emerged as targets for cancer therapy with developing selective inhibitors [98]. NTRK1, 2, and 3 gene rearrangements occur in several human cancers and they have been reported to have a 0.5% prevalence including TPM3-NTRK1 in CRCs [98]. A novel LMNA-NTRK1 rearrangement was reported in a metastatic CRC patient, who showed response to the pan-TRK inhibitor entrectinib [99].

Indication

HER2 IHC should be routinely performed in all inoperable, locally advanced, recurrent, and metastatic GCs and gastroesophageal junction (GEJ) cancers at the initial diagnosis and in the diagnosis of recurred or metastatic GCs. If the HER2 IHC results is equivocal of any cause, HER2 genetic testing by fluorescence in situ hybridization (FISH) or silver in situ hybridization (SISH) should be performed. Given that the majority of metastatic GCs are inoperable and need immediate first-line chemotherapy and they are predicted to progress very rapidly, HER2 IHC with or without SISH/FISH should be performed as quickly as possible [100]. Additionally, HER2 testing should be performed at relapse in patients with previously c-erbB2–negative tumors.

Other gene analyses such as FGFR2, HER2, ROS1, and NTRK are necessary in patients with pretreated metastatic GCs or CRCs for selecting targeted therapy. HER2 and MET amplification status would be helpful for predicting resistance to EGFR inhibitors.

Methodology

Method

Dual color FISH is recommended for gene amplification analysis. If possible, dual color SISH is also favored. Although both FISH and SISH, even if single-probe, showed good agreement for HER2 copy number testing in previous studies [101], it is widely accepted that SISH is a more preferred methodology than FISH because SISH is a bright-field methodology and enables pathologists to identify tumor area and HER2-positive area more rapidly, considering marked intratumoral HER2 heterogeneity [100,102]. Moreover, SISH slides can be stored for a longer period of time without bleaching than FISH slides.

ISH testing should be rejected and repeated if: (1) controls are not as expected, (2) the observer cannot find and count at least 20 invasive tumor cells, (3) >25% of signals are unscorable owing to weak signals, (4) >10% of signals occur over cytoplasm, (5) the nuclear resolution is poor, and (6) auto-fluorescence is strong [103].

Gene amplification status can also be examined by quantitative real-time PCR and digital PCR for target and reference gene fragments. Previous studies have demonstrated a close correlation between ISH results and quantitative PCR results using tissue or plasma samples, but with weak-to-moderate correlation [104]. This may be due to intratumoral heterogeneity and normal cell contamination. Therefore, ISH in cancer tissue samples is the gold standard method for gene amplification testing. PCR-based methods are not acceptable for confirmatory molecular diagnosis.

Type of specimen

Both surgical resection and biopsy can be used for ISH analysis. However, biopsies are more commonly available because advanced and metastatic gastrointestinal cancers are usually inoperable. Intratumoral heterogeneity of oncogenic gene amplification has been demonstrated by many researchers. Especially, heterogeneous HER2 expression is very common in GC and GEJ cancer, where upwards of 30% of HER2-positive GCs have been reported, and HER2 genetic status is closely correlated with HER2 expression status. Therefore, considering intratumoral HER2 heterogeneity, at least four to six biopsies by endoscopy are needed for sufficient and acceptable tests and to avoid false-negative results. The tissue microarray method is not recommended in routine clinical practice in pathology laboratories owing to HER2 heterogeneity [100,102].

Specimen requirements

In order to obtain acceptable ISH results, specimen quality is important which relies on excellent sample fixation and preparation procedures. Regarding the cold ischemia time, it is recommended to transfer the endoscopic biopsy specimens into fixatives within 20 minutes of excision and the surgical excision specimens into fixatives within 1 hour of resection. However, most of the surgical specimens cannot be subject to fixation within less than 1 hour of resection in daily practice; thus, the cold ischemia time should be as short as possible in each pathology laboratory. The Task Force for gastric HER2 testing recommended that laboratories have their own validation results of optimal cold ischemia time for biopsies and surgical specimens for appropriate tissue handling protocols [100]. The fixation should be done using a sufficient amount of 10% neutral buffered formalin and the duration of fixation should be 8–72 hours. Although it may be influenced by primary fixation or storage conditions, sections should not be used if cut >6 weeks earlier [103]. During the preparation, insufficient deparaffinization can result in nuclear bubbles in ISH slides, and over-digestion may result in nuclear holes [102].

Reporting

In metastatic GC patients, treatment must be planned with full knowledge of a patient’s HER2 status. When ISH signals are counted, it is recommended for the pathologists to use HER2 IHC slides as screening results and to count signals in the HER2 IHC-positive area in order to overcome heterogeneous HER2 reactivity [104]. At least 20 evaluable and non-overlapping cells from IHC 2+ areas should be counted initially. If ISH results indicate borderline amplification (HER2:CEP17 ratio 1.8–2.2), another 20 cells should be counted to reconfirm the HER2: CEP17 ratio. Only cells with at least one ISH signal for each probe should be counted if dual probes are used. The final diagnosis is defined as “ISH positive” if the HER2:CEP17 ratio is ≥2.0 and “ISH negative” if the HER2:CEP17 ratio is <2.0. The reports of HER2 testing should provide a confirmative HER2 status, and an “equivocal” result, which is defined in the recommendations of HER2 testing in breast cancer, should not be accepted in GC patients [100]. Testing must be reported as ‘indeterminate’ if the interpretation of the HER2 ISH result is precluded owing to technical issues such as poor specimen handling, significant tissue crushing artifact, and edge artifact [105].

Usually, the diagnostic criteria of gene amplification, including FGFR2 and MET in GC and HER2 and MET in CRC, have been defined as a target gene:reference gene ratio >2 [91], and the positivity criteria have been adopted from the recommendations of the gastric HER2 test. However, the HERACLES trial in metastatic CRC patients defined HER2-positivity criteria as tumors with a HER2 IHC 3+ score in more than 50% of cells or with HER2 IHC 2+ and a HER2:CEP17 >2 in more than 50% of cells by FISH [83]. The final molecular diagnosis should be determined using the validated criteria for each target gene and in each organ.

Validation of test

In initial performing HER2 testing in GC, 25–50 GC cases should be analyzed in parallel, using IHC and ISH, and the concordance rate of IHC and ISH should be >90% if equivocal IHC 2+ cases are excluded. Since HER2 testing and diagnosis in GC have unique features compared to that of breast cancer, initial set-up and validation must be independent of breast cancer protocols, performed by specifically trained persons in gastric HER2 testing, and documented in GC HER2 testing protocols [100,102]. Other gene amplification tests need to be validated for each gene and organ with full consideration of the differences among genes and organs.

Quality assurance

Each pathology laboratory should establish internal QA instructions for the ISH method and review all performed ISH analysis in regular QA meetings. It is recommended that all SISH slides and several representative images for FISH are stored. If possible, performing parallel analysis such as IHC is also recommended. The laboratory must maintain testing trends including positivity rates and scoring distributions, and record the possible reasons for their variation. All pathology laboratories should participate in external QA programs.

Epstein-Barr virus

Background

The EBV is a ubiquitous human herpes virus having a 172-kb DNA genome implicated in the etiology of many human malignancies [106]. The previous studies have demonstrated the presence of EBV in 2%–16% of conventional gastric adenocarcinomas worldwide, but the number of patients with EBV-associated GC is high because of the high incidence of GC, especially in Korea [7]. By TCGA results, EBV-positive GCs have a tendency of CIMP, but do not show a MSI-H phenotype or hMLH1 hypermethylation [25]. EBV-positive GCs were strongly associated with CDKN2A (p16INK4A) promoter hypermethylation and PIK3CA mutation [25]. The PIK3CA mutations were more dispersed in EBV-positive GCs, but localized in the kinase domain (exon 20) in EBV-negative cancers.

Morphologically, EBV-positive GC has characteristic abundant lymphoid stroma. By WHO classification, gastric carcinoma with lymphoid stroma is an uncommon subtype and is closely associated with the presence of EBV [1]. The high throughput study by the TCGA network revealed that IL-12 mediated immune cell signaling signatures were activated and PD-L1/2 mRNA was overexpressed in EBV-positive GCs [25]. Recent studies supported the relationship between the presence of EBV and aberrant immune checkpoint protein expression by demonstrating high PD-L1 protein expression in EBV-positive GCs [107,108]. Therefore, EBV-positive GCs are suggested to be good candidates for immune checkpoint inhibitor therapy.

Indication

EBV-associated gastric carcinoma has a characteristic heavy lymphoid stroma, but the extent and degree of lymphoid stroma is variable and EBV status cannot be predicted by histologic features only. Furthermore, although EBV and MSI are mutually exclusive in GCs, microsatellite unstable GCs are also associated with lymphocyte-rich histology [109]. Therefore, to determine the EBV status of GC patients, laboratory detection of EBV is necessary in the newly diagnosed GC patients.

Methodology

Method

Laboratory detection of EBV may be performed by several published methods [110]: (1) ISH identification of EBV-encoded small RNAs (EBER) directly in tumor cells; (2) EBV clonality assay by Southern blot analysis to distinguish latent form replicative infections; (3) EBV DNA amplification to detect viral DNA in patient tissues; (4) EBV viral load assays to quantitate EBV DNA in blood or body fluids to monitor disease status over time; (5) IHC for LMP1, EBNA1, EBNA2, LMP2A (latent state proteins of EBV), and BZLF1 (lytic state protein; so-called switch protein from lytic to latent state) to detect EBV-producing proteins and distinguish latent from replicative infections; (6) viral culture, which is possible but impractical for clinical use; (7) electron microscopy, which is also impractical; and (8) serology using VCA, EBNA, EA, and heterophile antibodies to monitor disease-association, -regression or -progression over time.

The presence or absence of EBV is examined by EBER ISH, and it is considered the gold standard for detecting and localizing latent EBV in tissue samples [111]. EBER transcripts are amplified, which represent a reliable target for determining the presence or absence of EBV in tissue sections by ISH. Commercially available EBER probes are labeled with biotin, digoxigenin, or fluorescein (Dako, Glostrup, Denmark; Enzo Diagnostics, Farmingdale, NY, USA; Kreatech Diagnostics, Amsterdam, The Netherlands; Novocastra Laboratories Ltd., Newcastle, UK; Shandon Lipshaw, Pittsburgh, PA, USA; Innogenex, San Ramon, CA; Ventana Medical Systems, Tucson, AZ, USA) [110]. The IHC method has some merits in that it is fast, convenient, and widely used compared with the ISH method. However, LMP1 is undetectable in EBV-associated carcinomas, and BZLF1 is the only characteristic of lytic viral replication [110].

Type of specimen

EBER ISH can be accomplished on paraffin sections from biopsy or surgical excision or on cytology preparations.

Specimen requirements

For EBER ISH, specimen quality is also important, which is dependent on good sample fixation and preparation procedures. The recommendations for specimen quality are the same as the other ISH analyses described above. The pathologists should select tumor sections with sufficient tumor cells to be included.

Reporting

EBER is usually detected uniformly in all of the tumor cells comprising an EBV-associated malignancy, but only focal EBER expression may be observed in tumors occasionally. EBER ISH signals are interpreted by microscopic examination and only the nuclear EBER positivity in tumor cells is defined as EBV-positive. Microscopic examination has additional advantages including evaluation of cell type and distribution of EBER signals.

Validation of test

The initial validation of EBER ISH is not different from that of the other ISH methods. It should be noted that nonspecific positivity in the cytoplasm of scattered normal epithelial cell is sometimes observed, and EBER-positive memory B cells are rarely found in some of the GC specimens.

Quality assurance

QA of EBER ISH is also similar to that of the other ISH methods. The internal and external QA programs are mandatory.

NEXT-GENERATION SEQUENCING CANCER PANEL

GC and CRC are genetically heterogeneous disorders driven by various genetic alterations [112,113]. Recently, the development of NGS has allowed a sharply increased sequencing capacity and rapid analysis of multiplexed samples [114]. NGS has cast a light on the comprehensive genetic aberration of the disease [115] and enabled the discovery of candidate genes as potential targets in cancer therapy [116]. Through the recent development of molecular genomics, molecular profiling of gastrointestinal carcinoma by large-scale cancer genomics projects has also been performed [25,26]. The TCGA research network completed the genomic sequencing of CRC and classified it based on the molecular feature [25,26].

In the TCGA report, GCs are divided into two classes: the hypermutated and nonhypermutated tumor. The non-hypermutated tumor includes genomically stable and chromosomally unstable subtypes. EBV-positive and MSI-H subtypes represent the hypermutated tumor and have frequent mutations in PIK3CA and ARID1A. Other studies have discovered that RHOA and CDH1 are possible driver genes in diffuse-type GC [117,118]. The gene mutations that contribute to gastric carcinoma, which have been revealed in previous large-scale studies, are listed in Table 2. CRC was also categorized into the hypermutated and the non-hypermutated tumor. The hypermutated tumors are characterized by elevated levels of MSI and defects in DNA MMR mechanisms. An activating mutation of BRAF is frequently presented in the hypermutated tumor [119,120]. Recurrent mutation of TP53, KRAS, APC, and PIK3CA has been consistently reported in previous studies and it is notable that the significantly frequent KRAS mutation is identified in non-hypermutated tumors (Table 3) [114,119,121].

Table 2.

Recurrent somatic genetic alteration in gastric cancer analyzed using next-generation sequencing

Gene	Classification	Core pathway	Process	Mutational rate (%)			Reference
				Previous study	Hypermutated tumora	Nonhypermutated tumora
TP53	TSG	Cell cycle/apoptosis, DNA damage control	Cell survival	14–59	35	50	27,116–118,123–127
PIK3CAb	Oncogene	PI3K-AKT	Cell survival	7–36	40	12	27,116–118,123–127
CDH1c	TSG	APC	Cell fate	4–36	-	11	27,116–118,124–126
ARID1Ab	TSG	Chromatin modification	Cell fate	8–27	44	14	27,116,118,123–126
PTEN	TSG	PI3K-AKT	Cell survival	0–27	13	-	27,116,123,125,127
KRAS	Oncogene	RAS/RAF	Cell survival	0–27	19	6	27,116,118,125,127
RHOAc	Oncogene	RHO/ROCK	Cell survival	0–23	-	6	27,116,118
APC	TSG	APC	Cell fate	3–14	-	7	27,116,118,123,124
ERBB3	Oncogene	RTK	Cell survival	0–10	25	-	27,116
ERBB2	Oncogene	RTK	Cell survival	2–9	-	3	27,116,118,126,127
CTNNB1	Oncogene	APC	Cell fate	2–9	-	4	27,116,118,124
MET	Oncogene	RTK	Cell survival	0–9		-	116,127
FBXW7	TSG	NOTCH	Cell fate	2–6	24	-	27,118,127
SMAD4	TSG	TGF-β	Cell survival	4–6	-	8	27,118
EGFR	Oncogene	RTK	Cell survival	0–6	-	-	27,116,127
NRAS	Oncogene	RAS/RAF	Cell survival	0–5	-	-	116,125,127

TSG, tumour suppressor gene; PI3K, phosphoinositide 3-kinase; RTK, receptor tyrosine kinase; TGF-β, transforming growth factor β.

^aData of mutation rates are from The Cancer Genome Atlas database; [25]

^bMore frequently mutated gene in gastric cancer with microsatellite instability–high frequency feature or Epstein-Barr virus positivity;

^cMore frequently mutated gene in gastric cancer with diffuse type of Lauren classification.

Table 3.

Recurrent somatic genetic alteration in colorectal cancer analyzed using next-generation sequencing

Gene	Classification	Core pathway	Process	Mutational rate (%)			Reference
				Previous study	Hypermutated tumora	Nonhypermutated tumora
TP53b	TSG	Cell cycle/apoptosis, DNA damage control	Cell survival	27–65	20	60	119–121,128,129
KRASb	Oncogene	RAS/RAF	Cell survival	33–58	30	43	119–121,128–131
APCb,c	TSG	APC	Cell fate	40–56	51	81	121,129
PIK3CAb	Oncogene	PI3K-AKT	Cell survival	14–20	-	18	119,120,128,129,131
BRAFc	Oncogene	RAS/RAF	Cell survival	5–14	46	-	119,120,128–131
PTEN	TSG	PI3K-AKT	Cell survival	2–13	-	-	119,128,129
EGFR	Oncogene	RTK	Cell survival	0–11	-	-	128,129,131
SMAD4b	TSG	TGF-β	Cell survival	2–11	-	10	119,121,128,129
FBXW7b	TSG	NOTCH	Cell fate	4–10	-	11	119,120,128,129
NRAS	Oncogene	RAS	Cell survival	2–7	-	9	119,120,128–131
MET	Oncogene	RTK	Cell survival	2–4	-	-	119,120
CTNNB1	Oncogene	APC	Cell fate	1–4	-	5	121,128,129
AKT1	Oncogene	PI3K	Cell survival	1–4	-	-	119,128,129
ERBB2	Oncogene	RTK	Cell survival	1–3	-	-	128,129
ALK	Oncogene	RTK	Cell survival	1–2	-	-	120,128,129
MAP2K1	Oncogene	RAS/RAF	Cell survival	0–2	-	-	119–121,128

TSG, tumour suppressor gene; PI3K, phosphoinositide 3-kinase; RTK, receptor tyrosine kinase; TGF-β, transforming growth factor β.

^aData of mutation rates are from The Cancer Genome Atlas database; [26]

^bMore frequently mutated gene in nonhypermutated colorectal cancer;

^cMore frequently mutated gene in hypermutated colorectal cancer.

In the era of precision medicine, the clinical implication of NGS for multiple biomarker tests has been consistently required. With the aid of TCGA data which highlighted relevant genetic alterations and driver mutations linked to its biological pathway, various panels for multi-gene profile of carcinoma have been suggested. Multi-gene panels should identify a clinically actionable genetic aberration including variants linked to molecular classification, prediction of treatment response, and current/future target of therapy [122]. For instance, the Ion AmpliSeq Colon and Lung Cancer Research Panel includes more than 20 genes, such as RTK genes, RTK signaling genes, and other well-known cancer-related genes. However, these panels have not been fully validated using clinical samples and their inter-laboratory reproducibility has not been shown. Hence, the search for an ideal cancer marker panel and its validation by multi-centered and large-scale studies is still needed.

CONCLUSION

Remarkable developments in molecular and genomic techniques have increased the importance of molecular classification or grading in gastrointestinal cancers. Molecular testing is necessary for screening hereditary disease, predicting patient prognosis, and predicting the responses to targeted therapy. Standardization and quality control of the pre-analytic, analytic, and postanalytic steps of each molecular test are essential for reliable diagnostic results. In particular, the pathologists are responsible for the selection of appropriate specimen, with sufficient tumor cell quantity and well-preserved nucleic acids, authorizing the test results, and providing reliable molecular and genomic information to the clinician. Because the validation of the test, diagnostic criteria, and interpretation are not the same for each gene or each tumor, pathologists with subspecialty expertise are necessary. Therefore, the pathologists must obtain recent and integrated knowledge, and accumulate their experience in molecular testing.